EMBRYOPSIDA Pirani & Prado
Gametophyte dominant, independent, multicellular, initially ±globular, not motile, branched; showing gravitropism; glycolate oxidase +, glycolate metabolism in leaf peroxisomes [glyoxysomes], acquisition of phenylalanine lysase* [PAL], flavonoid synthesis*, microbial terpene synthase-like genes +, triterpenoids produced by CYP716 enzymes, CYP73 and phenylpropanoid metabolism [development of phenolic network], xyloglucans in primary cell wall, side chains charged; plant poikilohydrous [protoplasm dessication tolerant], ectohydrous [free water outside plant physiologically important]; thalloid, leafy, with single-celled apical meristem, tissues little differentiated, rhizoids +, unicellular; chloroplasts several per cell, pyrenoids 0; centrioles/centrosomes in vegetative cells 0, microtubules with γ-tubulin along their lengths [?here], interphase microtubules form hoop-like system; metaphase spindle anastral, predictive preprophase band + [with microtubules and F-actin; where new cell wall will form], phragmoplast + [cell wall deposition centrifugal, from around the anaphase spindle], plasmodesmata +; antheridia and archegonia +, jacketed*, surficial; blepharoplast +, centrioles develop de novo, bicentriole pair coaxial, separate at midpoint, centrioles rotate, associated with basal bodies of cilia, multilayered structure + [4 layers: L1, L4, tubules; L2, L3, short vertical lamellae] (0), spline + [tubules from L1 encircling spermatid], basal body 200-250 nm long, associated with amorphous electron-dense material, microtubules in basal end lacking symmetry, stellate array of filaments in transition zone extended, axonemal cap 0 [microtubules disorganized at apex of cilium]; male gametes [spermatozoids] with a left-handed coil, cilia 2, lateral, asymmetrical; oogamy; sporophyte +*, multicellular, growth 3-dimensional*, cuticle +*, plane of first cell division transverse [with respect to long axis of archegonium/embryo sac], sporangium and upper part of seta developing from epibasal cell [towards the archegonial neck, exoscopic], with at least transient apical cell [?level], initially surrounded by and dependent on gametophyte, placental transfer cells +, in both sporophyte and gametophyte, wall ingrowths develop early; suspensor/foot +, cells at foot tip somewhat haustorial; sporangium +, single, terminal, dehiscence longitudinal; meiosis sporic, monoplastidic, MTOC [= MicroTubule Organizing Centre] associated with plastid, sporocytes 4-lobed, cytokinesis simultaneous, preceding nuclear division, quadripolar microtubule system +; wall development both centripetal and centrifugal, 1000 spores/sporangium, sporopollenin in the spore wall* laid down in association with trilamellar layers [white-line centred lamellae; tripartite lamellae]; plastid transmission maternal; nuclear genome [1C] <1.4 pg, main telomere sequence motif TTTAGGG, KNOX1 and KNOX2 [duplication] and LEAFY genes present, ethylene involved in cell elongation; chloroplast genome with close association between trnLUAA and trnFGAA genes [precursors for starch synthesis], tufA, minD, minE genes moved to nucleus; mitochondrial trnS(gcu) and trnN(guu) genes +.
Many of the bolded characters in the characterization above are apomorphies of more or less inclusive clades of streptophytes along the lineage leading to the embryophytes, not apomorphies of crown-group embryophytes per se.
All groups below are crown groups, nearly all are extant. Characters mentioned are those of the immediate common ancestor of the group,  contains explanatory material, () features common in clade, exact status unclear.
Sporophyte well developed, branched, branching dichotomous, potentially indeterminate; hydroids +; stomata on stem; sporangia several, terminal; spore walls not multilamellate [?here].
II. TRACHEOPHYTA / VASCULAR PLANTS
Sporophyte long lived, cells polyplastidic, photosynthetic red light response, stomata open in response to blue light; plant homoiohydrous [water content of protoplasm relatively stable]; control of leaf hydration passive; plant endohydrous [physiologically important free water inside plant]; PIN[auxin efflux facilitators]-mediated polar auxin transport; (condensed or nonhydrolyzable tannins/proanthocyanidins +); borate cross-linked rhamnogalactan II, xyloglucans with side chains uncharged [?level], in secondary walls of vascular and mechanical tissue; lignins +; roots +, often ≤1 mm across, root hairs and root cap +; stem apex multicellular [several apical initials, no tunica], with cytohistochemical zonation, plasmodesmata formation based on cell lineage; vascular development acropetal, tracheids +, in both protoxylem and metaxylem, G- and S-types; sieve cells + [nucleus degenerating]; endodermis +; stomata numerous, involved in gas exchange; leaves +, vascularized, spirally arranged, blades with mean venation density ca 1.8 mm/mm2 [to 5 mm/mm2], all epidermal cells with chloroplasts; sporangia in strobili, sporangia adaxial, columella 0; tapetum glandular; sporophyte-gametophyte junction lacking dead gametophytic cells, mucilage, ?position of transfer cells; MTOCs not associated with plastids, basal body 350-550 nm long, stellate array in transition region initially joining microtubule triplets; archegonia embedded/sunken [only neck protruding]; embryo suspensor +, shoot apex developing away from micropyle/archegonial neck [from hypobasal cell, endoscopic], root lateral with respect to the longitudinal axis of the embryo [plant homorhizic].[MONILOPHYTA + LIGNOPHYTA]
Sporophyte growth ± monopodial, branching spiral; roots endomycorrhizal [with Glomeromycota], lateral roots +, endogenous; G-type tracheids +, with scalariform-bordered pits; leaves with apical/marginal growth, venation development basipetal, growth determinate; sporangium dehiscence by a single longitudinal slit; cells polyplastidic, MTOCs diffuse, perinuclear, migratory; blepharoplasts +, paired, with electron-dense material, centrioles on periphery, male gametes multiciliate; nuclear genome [1C] 7.6-10 pg [mode]; chloroplast long single copy ca 30kb inversion [from psbM to ycf2]; mitochondrion with loss of 4 genes, absence of numerous group II introns; LITTLE ZIPPER proteins.
Sporophyte woody; stem branching axillary, buds exogenous; lateral root origin from the pericycle; cork cambium + [producing cork abaxially], vascular cambium bifacial [producing phloem abaxially and xylem adaxially].
SEED PLANTS† / SPERMATOPHYTA†
Growth of plant bipolar [plumule/stem and radicle/root independent, roots positively geotropic]; plants heterosporous; megasporangium surrounded by cupule [i.e. = unitegmic ovule, cupule = integument]; pollen lands on ovule; megaspore germination endosporic, female gametophyte initially retained on the plant, free-nuclear/syncytial to start with, walls then coming to surround the individual nuclei, process proceeding centripetally.
EXTANT SEED PLANTS
Plant evergreen; nicotinic acid metabolised to trigonelline, (cyanogenesis via tyrosine pathway); microbial terpene synthase-like genes 0; primary cell walls rich in xyloglucans and/or glucomannans, 25-30% pectin [Type I walls]; lignin chains started by monolignol dimerization [resinols common], particularly with guaiacyl and p-hydroxyphenyl [G + H] units [sinapyl units uncommon, no Maüle reaction]; roots often ≥1 mm across, stele diarch to pentarch, xylem and phloem originating on alternating radii, cork cambium deep seated, gravitropism response fast; stem apical meristem complex [with quiescent centre, etc.], plasmodesma density in SAM 1.6-6.2[mean]/μm2 [interface-specific plasmodesmatal network]; eustele +, protoxylem endarch, endodermis 0; wood homoxylous, tracheids and rays alone, tracheid/tracheid pits circular, bordered; mature sieve tube/cell lacking functioning nucleus, sieve tube plastids with starch grains; phloem fibres +; cork cambium superficial; leaf nodes 1:1, a single trace leaving the vascular sympodium; leaf vascular bundles amphicribral; guard cells the only epidermal cells with chloroplasts, stomatal pore with active opening in response to leaf hydration, control by abscisic acid, metabolic regulation of water use efficiency, etc.; branching by axillary buds, exogenous; prophylls two, lateral; leaves with petiole and lamina, development basipetal, lamina simple; sporangia borne on sporophylls; spores not dormant; microsporophylls aggregated in indeterminate cones/strobili; grains monosulcate, aperture in ana- position [distal], primexine + [involved in exine pattern formation with deposition of sporopollenin from tapetum there], exine and intine homogeneous, exine alveolar/honeycomb; ovules with parietal tissue [= crassinucellate], megaspore tetrad linear, functional megaspore single, chalazal, sporopollenin 0; gametophyte ± wholly dependent on sporophyte, development initially endosporic [apical cell 0, rhizoids 0, etc.]; male gametophyte with tube developing from distal end of grain, male gametes two, developing after pollination, with cell walls; embryo cellular ab initio, suspensor short-minute, embryonic axis straight [shoot and root at opposite ends], primary root/radicle produces taproot [= allorhizic], cotyledons 2; embryo ± dormant; chloroplast ycf2 gene in inverted repeat, trans splicing of five mitochondrial group II introns, rpl6 gene absent; ??whole nuclear genome duplication [ζ/zeta duplication event], 2C genome size (0.71-)1.99(-5.49) pg, two copies of LEAFY gene, PHY gene duplications [three - [BP [A/N + C/O]] - copies], 5.8S and 5S rDNA in separate clusters.
IID. ANGIOSPERMAE / MAGNOLIOPHYTA
Lignans, O-methyl flavonols, dihydroflavonols, triterpenoid oleanane, apigenin and/or luteolin scattered, [cyanogenesis in ANA grade?], lignin also with syringyl units common [G + S lignin, positive Maüle reaction - syringyl:guaiacyl ratio more than 2-2.5:1], hemicelluloses as xyloglucans; root cap meristem closed (open); pith relatively inconspicuous, lateral roots initiated immediately to the side of [when diarch] or opposite xylem poles; epidermis probably originating from inner layer of root cap, trichoblasts [differentiated root hair-forming cells] 0, hypodermis suberised and with Casparian strip [= exodermis]; shoot apex with tunica-corpus construction, tunica 2-layered; starch grains simple; primary cell wall mostly with pectic polysaccharides, poor in mannans; tracheid:tracheid [end wall] plates with scalariform pitting, wood parenchyma +; sieve tubes enucleate, sieve plates with pores (0.1-)0.5-10< µm across, cytoplasm with P-proteins, not occluding pores of plate, companion cell and sieve tube from same mother cell; ?phloem loading/sugar transport; nodes 1:?; dark reversal Pfr → Pr; protoplasm dessication tolerant [plant poikilohydric]; stomata randomly oriented, brachyparacytic [ends of subsidiary cells ± level with ends of guard cells], outer stomatal ledges producing vestibule, reduction in stomatal conductance with increasing CO2 concentration; lamina formed from the primordial leaf apex, margins toothed, development of venation acropetal, overall growth ± diffuse, secondary veins pinnate, fine venation hierarchical-reticulate, (1.7-)4.1(-5.7) mm/mm2, vein endings free; flowers perfect, pedicellate, ± haplomorphic, protogynous; parts free, numbers variable, development centripetal; P = T, petal-like, each with a single trace, outer members not sharply differentiated from the others, not enclosing the floral bud; A many, filament not sharply distinguished from anther, stout, broad, with a single trace, anther introrse, tetrasporangiate, sporangia in two groups of two [dithecal], each theca dehiscing longitudinally by a common slit, ± embedded in the filament, walls with at least outer secondary parietal cells dividing, endothecium +, cells elongated at right angles to long axis of anther; tapetal cells binucleate; microspore mother cells in a block, microsporogenesis successive, walls developing by centripetal furrowing; pollen subspherical, tectum continuous or microperforate, ektexine columellate, endexine restricted to the apertural regions, thin, compact, intine in apertural areas thick, orbicules +, pollenkitt +; nectary 0; carpels present, superior, free, several, spiral, ascidiate [postgenital occlusion by secretion], stylulus at most short [shorter than ovary], hollow, cavity not lined by distinct epidermal layer, stigma ± decurrent, carinal, dry; suprastylar extragynoecial compitum +; ovules few [?1]/carpel, marginal, anatropous, bitegmic, micropyle endostomal, outer integument 2-3 cells across, often largely subdermal in origin, inner integument 2-3 cells across, often dermal in origin, parietal tissue 1-3 cells across, nucellar cap?; megasporocyte single, hypodermal, functional megaspore lacking cuticle; female gametophyte lacking chlorophyll, four-celled [one module, egg and polar nuclei sisters]; ovule not increasing in size between pollination and fertilization; pollen grains bicellular at dispersal, germinating in less than 3 hours, siphonogamy, pollen tube unbranched, growing towards the ovule, between cells, growth rate (ca 10-)80-20,000 µm h-1, tube apex of pectins, wall with callose, lumen with callose plugs, penetration of ovules via micropyle [porogamous], whole process takes ca 18 hours, distance to first ovule 1.1-2.1 mm; male gametophytes tricellular, gametes 2, lacking cell walls, ciliae 0, double fertilization +, ovules aborting unless fertilized; fruit indehiscent, P deciduous; mature seed much larger than fertilized ovule, small [<5 mm long], dry [no sarcotesta], exotestal; endosperm +, ?diploid [one polar nucleus + male gamete], cellular, development heteropolar [first division oblique, micropylar end initially with a single large cell, divisions uniseriate, chalazal cell smaller, divisions in several planes], copious, oily and/or proteinaceous, embryo short [<¼ length of seed]; plastid and mitochondrial transmission maternal; Arabidopsis-type telomeres [(TTTAGGG)n]; nuclear genome [2C] (0.57-)1.45(-3.71) [1 pg = 109 base pairs], ??whole nuclear genome duplication [ε/epsilon event]; ndhB gene 21 codons enlarged at the 5' end, single copy of LEAFY and RPB2 gene, knox genes extensively duplicated [A1-A4], AP1/FUL gene, palaeo AP3 and PI genes [paralogous B-class genes] +, with "DEAER" motif, SEP3/LOFSEP and three copies of the PHY gene, [PHYB [PHYA + PHYC]]; chloroplast IR expansions, chlB, -L, -N, trnP-GGG genes 0.
[NYMPHAEALES [AUSTROBAILEYALES [[CHLORANTHALES + MAGNOLIIDS] [MONOCOTS [CERATOPHYLLALES + EUDICOTS]]]]]: wood fibres +; axial parenchyma diffuse or diffuse-in-aggregates; pollen monosulcate [anasulcate], tectum reticulate-perforate [here?]; ?genome duplication; "DEAER" motif in AP3 and PI genes lost, gaps in these genes.
[AUSTROBAILEYALES [[CHLORANTHALES + MAGNOLIIDS] [MONOCOTS [CERATOPHYLLALES + EUDICOTS]]]]: phloem loading passive, via symplast, plasmodesmata numerous; vessel elements with scalariform perforation plates in primary xylem; essential oils in specialized cells [lamina and P ± pellucid-punctate]; tension wood + [reaction wood: with gelatinous fibres, G-fibres, on adaxial side of branch/stem junction]; anther wall with outer secondary parietal cell layer dividing; tectum reticulate; nucellar cap + [character lost where in eudicots?]; 12BP [4 amino acids] deletion in P1 gene.
[[CHLORANTHALES + MAGNOLIIDS] [MONOCOTS [CERATOPHYLLALES + EUDICOTS]]] / MESANGIOSPERMAE: benzylisoquinoline alkaloids +; sesquiterpene synthase subfamily a [TPS-a] [?level], polyacetate derived anthraquinones + [?level]; outer epidermal walls of root elongation zone with cellulose fibrils oriented transverse to root axis; P more or less whorled, 3-merous [?here]; pollen tube growth intra-gynoecial; extragynoecial compitum 0; carpels plicate [?here]; embryo sac monosporic [spore chalazal], 8-celled, bipolar [Polygonum type], antipodal cells persisting; endosperm triploid.
[MONOCOTS [CERATOPHYLLALES + EUDICOTS]]: (veins in lamina often 7-17 mm/mm2 or more [mean for eudicots 8.0]); (stamens opposite [two whorls of] P); (pollen tube growth fast).
MONOCOTYLEDONS / MONOCOTYLEDONEAE / LILIANAE Takhtajan
Plant herbaceous, perennial, rhizomatous, growth sympodial; non-hydrolyzable tannins [(ent-)epicatechin-4] +, neolignans 0, CYP716 triterpenoid enzymes 0, benzylisoquinoline alkaloids 0, hemicelluloses as xylan, cell wall also with (1->3),(1->4)-ß-D-MLGs [Mixed-Linkage Glucans]; root epidermis developed from outer layer of cortex; endodermal cells with U-shaped thickenings; cork cambium [uncommon] superficial; stele oligo- to polyarch, medullated [with prominent pith], lateral roots arise opposite phloem poles; stem primary thickening meristem +; vascular development bidirectional, bundles scattered, (amphivasal), vascular cambium 0 [bundles closed]; tension wood 0; vessel elements in roots with scalariform and/or simple perforations; tracheids only in stems and leaves; sieve tube plastids with cuneate protein crystals alone; ?nodal anatomy; stomata oriented parallel to the long axis of the leaf, in lines; prophyll single, adaxial; leaf blade linear, main venation parallel, of two or more size classes, the veins joining successively from the outside at the apex and forming a fimbrial vein, transverse veinlets +, unbranched [leaf blade characters: ?level], vein/veinlet endings not free, margins entire, Vorläuferspitze +, base broad, ensheathing the stem, sheath open, petiole 0; inflorescence terminal, racemose; flowers 3-merous [6-radiate to the pollinator], polysymmetric, pentacyclic; P = T = 3 + 3, all with three traces, median T of outer whorl abaxial, aestivation open, members of whorls alternating, [pseudomonocyclic, each T member forming a sector of any tube]; stamens = and opposite each T member [A/T primordia often associated, and/or A vascularized from T trace], anther and filament more or less sharply distinguished, anthers subbasifixed, wall with two secondary parietal cell layers, inner producing the middle layer [monocot type]; pollen reticulations coarse in the middle, finer at ends of grain, infratectal layer granular; G , with congenital intercarpellary fusion, opposite outer tepals [thus median member abaxial], placentation axile; compitum +; ovule with outer integument often largely dermal in origin, parietal tissue 1 cell across; antipodal cells persistent, proliferating; seed small to medium sized [mean = 1.5 mg], testal; embryo long, cylindrical, cotyledon 1, apparently terminal [i.e. bend in embryo axis], with a closed sheath, unifacial [hyperphyllar], both assimilating and haustorial, plumule apparently lateral; primary root unbranched, not very well developed, stem-borne roots numerous [= homorhizic], hypocotyl short, (collar rhizoids +); no dark reversion Pfr → Pr; nuclear genome [2C] (0.7-)1.29(-2.35) pg, duplication producing monocot LOFSEP and FUL3 genes [latter duplication of AP1/FUL gene], PHYE gene lost.
[ALISMATALES [PETROSAVIALES [[DIOSCOREALES + PANDANALES] [LILIALES [ASPARAGALES + COMMELINIDS]]]]]: ethereal oils 0; (trichoblasts in vertical files, proximal cell smaller); raphides + (druses 0); leaf blade vernation supervolute-curved or variants, (margins with teeth, teeth spiny); endothecium develops directly from undivided outer secondary parietal cells; tectum reticulate with finer sculpture at the ends of the grain, endexine 0; septal nectaries + [intercarpellary fusion postgenital].
[PETROSAVIALES [[DIOSCOREALES + PANDANALES] [LILIALES [ASPARAGALES + COMMELINIDS]]]]: cyanogenic glycosides uncommon; starch grains simple, amylophobic; leaf blade developing basipetally from hyperphyll/hypophyll junction; epidermis with bulliform cells [?level]; stomata anomocytic, (cuticular waxes as parallel platelets); colleters 0.
[[DIOSCOREALES + PANDANALES] [LILIALES [ASPARAGALES + COMMELINIDS]]]: nucellar cap 0; ovary inferior; endosperm nuclear [but variation in most orders].
[LILIALES [ASPARAGALES + COMMELINIDS]]: (inflorescence branches cymose); protandry common.
[ASPARAGALES + COMMELINIDS]: style long; whole nuclear genome duplication [τ/tau event].
Age. This node has been dated to 118-116 Ma (Bremer 2000b; Leebens-Mack et al. 2005). Other estimates are are around 159 Ma (Paterson et al. 2004), ca 135.6 Ma (Tank et al. 2015: Table S1), ca 128 Ma (G.-Q. Zhang et al. 2017: sampling), (133.9-)123.6(-113.1) Ma (Eguchi & Tamura 2016), ca 122 Ma (Janssen & Bremer 2004), (126-)122(-98) Ma (Merckx et al. 2008a), about 121 Ma in Foster et al. (2016a: q.v. for details), (112-)107, 98(-93) Ma (Wikström et al. 2001) and ca 133.1 and 118.6 Ma (Magallón & Castillo 2009); ages a mere 76.6 or 75.4 Ma in Xue et al. (2012) and 88.9-78.2 Ma in Good-Avila (2006), (130-)121(-116) or (121-)115(-110) Ma in Hertweck et al. (2015), a group of similar estimates, 116-94 Ma in Mennes et al. (2013, see also 2015), about 120-90 Ma in S. Chen et al. (2013: conflicting estimates), and about 114.6 Ma in Magallón et al. (2015). Some ages are older than estimates of that of the [Liliales [Asparagales + commelinids]] node.
Evolution: Genes & Genomes. A genome duplication, the τ/tau genome duplication event, may be pegged to the ancestor of the monocots as a whole (Jiao et al. 2014), or at least to the clade [Asparagales + commelinids] (Deng et al. 2015); the latter position seems more likely (McKain et al. 2016; see also Olsen et al. 2016; H. T. Lee et al. 2016). There may have been 5 (Murat et al. 2017) or 7 (Ming et al. 2015) preduplication protochromosomes, so what happened may be x = 7 → x = 14 (tetraploidy: τ/tau genome duplication event) (Ming et al. 2015: pineapple) or x = 5 → x = 10 (Murat et al. 2017). P. Soltis and Soltis (2016) note that uncertainty over exactly where this event should be placed makes it difficult to think about any evolutionary implications it might have. Note that the ORSAγ duplication event (Landis et al. 2018) is placed two nodes down the tree at the [[Dioscoreales + Pandanales] [Liliales...]] node.
ASPARAGALES Link - Main Tree.
Chelidonic acid +, steroidal saponins 0 [exact position where?]; (velamen +), root hairs from unmodified rhizodermal cells; anthers longer than wide; microsporogenesis simultaneous; ovules many/carpel; seeds with phytomelan (0), exotestal, tegmen not persistent; endosperm helobial; mitochondrial sdh3 gene lost. - 14 families, 1,122 genera, 36,265 species.
Includes Amaryllidaceae, Asparagaceae (see Agavoideae, Aphyllanthoideae, Asparagoideae, Brodiaeoideae, Lomandroideae, Nolinoideae and Scilloideae), Asphodelaceae, Asteliaceae, Blandfordiaceae, Boryaceae, Doryanthaceae, Hypoxidaceae, Iridaceae, Ixioliriaceae, Lanariaceae, Orchidaceae, Tecophilaeaceae, Xeronemataceae.
Note: In all node characterizations, boldface denotes a possible apomorphy, (....) denotes a feature the exact status of which in the clade is uncertain, [....] includes explanatory material; other text lists features found pretty much throughout the clade. Note that the precise node to which many characters, particularly the more cryptic ones, should be assigned is unclear. This is partly because homoplasy is very common, in addition, basic information for all too many characters is very incomplete, frequently coming from taxa well embedded in the clade of interest and so making the position of any putative apomorphy uncertain. Then there are the not-so-trivial issues of how character states are delimited and ancestral states are reconstructed (see above).
Age. Crown group Asparagales may be ca 125.3 Ma (Tank et al. 2015: Table S2; see also C. Q. Tang et al. 2016), ca 119 Ma (Janssen & Bremer 2004) or (118-)112, 110(-106) Ma (Hertweck et al. (2015; see also Givnish et al. 2015, 2016a), although Wikström et al. (2001: note topology) had suggested dates of 101-92 My; Magallón and Castillo (2009) suggested ages of ca 112.6 Ma and Bell et al. (2010) ages of (114-)103, 92(-83) Ma. Other estimates are (127-)119(-101) Ma in Merckx et al. (2008a), 96-93 Ma or 113-63 Ma in Mennes et al. (2013, 2015 respectively), 101-93 or 85.1 Ma in S. Chen et al. (2013), about 109 Ma in Magallón et al. (2015) and (125.8-)112.9(-98.4) Ma in Eguchi and Tamura (2016). The rather young age in Smith et al. (2008) is (95.6-)90.3(-85) Ma and that in D.-F. Xie et al. (2020) is (78.3-)74.6(-70.8) Ma, but the lowest suggested age seems to be 69-60 Ma (Good-Avila et al. 2006). Ages in Serna-Sánchez et al. (2021: Orchidaceae sister to the rest?) are ca 123.6 (strict clock) or ca 113.7 Ma (relaxed clock) and in C. I. Smith et al. (2021) they are (124.0-)104.0(-83.7) Ma.
Silvestro et al. (2020) estimate the time-of-origin of Orchidaceae to be ca 137.7 Ma.
Evolution: Divergence & Distribution. S. Chen et al. (2013) give age estimates for many nodes in Asparagales in particular, but differences between the two methods that they used were often substantial, the older ages (from BEAST) being about half as much again as the younger age (PATHd8) in a third or so of the cases.
Asparagales may have the highest diversification rate in the monocots, about the same as Poales, but in both the rate is little over half that of Lamiales, the angiosperm clade with the highest rate (Magallón & Castillo 2009); Magallón and Sanderson (2001) did not give estimates for the group. Within the clade, the diversity of Orchidaceae is remarkable, but to understand that diversity it makes as much sense to focus on clades within Orchidaceae as on the family as a whole (e.g. Givnish et al. 2015; see below). Endress (2011a) thought that an inferior ovary might be a key innovation in Asparagales, and Rudall (2001a, see also 2002, 2003a) included an inferior ovary as a synapomorphy of the order, noting that in "higher" Asparagales there might be a reversal to superior ovaries that is associated with the presence of infralocular septal nectaries (as in Xanthorrhoea and Johnsonia (Asphodelaceae-Xanthorrhoeoideae and -Hemerocallidoideae). Tobe et al. (2018) thought that inferior ovaries had evolved two nodes down the tree (see the [[Dioscoreales + Pandanales] [Liliales...]] node), but in either case inferior ovaries are scattered through the Asparagales and fitting ovary evolution to the tree is difficult; ovary position is a very labile character.
Some 2,550 species in five major clades of Asparagales in southern Africa, e.g. in Iridaceae and Asphodelaceae, but not Orchidaceae-Epidendroideae, make the group notably diverse there (Johnson 2010).
Plant-Animal Interactions. Food plants of caterpillars of the [Heteropterinae-Trapezetinae-Hesperiinae] clade of skippers are common here, but most are found on Poaceae (Warren et al. 2009).
Bacterial/Fungal Associations. Asparagales commonly have Arum-type arbuscular mycorrhizae where the hyphae are intercellular, and also form coils, pelotons and particularly branched arbuscules within cells, while in Liliales these mycorrhizae are commonly Paris-type with intercellular hyphae that form coiled structures between the cells (F. A. Smith & Smith 1997; Rasmussen & Rasmussen 2014).
Genes & Genomes. Asparagales have a very wide spread in genome sizes - 0.3-82.2 pg (1C: Leitch & Leitch 2013). For cytology here, see Tamura (1995).
There has been much duplication of genes in the TEOSINTE BRANCHED and PROLIFERATION CELL FACTOR gene families in this clade, and they are commonly expressed in the ovary/fruit and sometimes in the leaf, etc., in Orchidaceae and Hypoxidaceae (see below for what also goes on in Orchidaceae). Interestingly, CYC and TB1 genes (the former are not duplicated) seem not to be involved in the development of monosymmetry in the flowers of Asparagales, unlike their roles in Commelinales, Zingiberales and Liliales (Madrigal et al. 2017).
Chemistry, Morphology, etc.. For fructan sugar accumulation, quite common outside Orchidaceae, see Pollard (1982). Storage mannans in the vegetative tissues are reported from Asphodelaceae-Asphodeloideae, Amaryllidaceae and Orchidaceae; they are uncommon elsewhere (Meier & Reid 1982). There is no starch in the chloroplasts of guard cells of members of Amaryllidaceae, Iridaceae, and "Liliaceae" (= Allium) and no chloroplasts at all in those of Paphiopedilum (Orchidaceae) (D'Amelio & Zieger 1988; Willmer & Fricker 1996).
There are three-trace tepals in Orchidaceae, Amaryllidaceae-Amaryllidoideae and -Agapanthoideae, Iridaceae, Asphodelaceae-Asphodeloideae (but not Kniphofia, Ashpodelus) and -Hemerocallidoideae, Asparagaceae-Agavoideae; one-trace tepals in Amaryllidaceae-Allioideae and Asparagaceae-Nolinoideae (but not Maianthemum stellatum), -Aphyllanthoideae, and -Asparagoideae. Asparagaceae-Scilloideae have tepals with both one and three traces, Urginea (= Drimia) even having five traces in the outer whorl and three in the inner (Chatin 1920; Carpenter 1938). Where changes in microsporogenesis are to be placed on the tree is not clear.
For flavonoids, see C. A. Williams et al. (1988), for general morphology, see Rudall (2003a), for root morphology, see Kauff et al. (2000), for cladodes, see Schlittler (1953b), for inflorescences, see Schlittler (1953a), for pollen of Japanese representatives, see Handa et al. (2001), for ovule and seed, see Shamrov (1999a) and Oganezova (2000a, b), and for the distribution of taxa with phytomelan and/or with baccate fruits, see Rasmussen et al. (2006).
Phylogeny. For a discussion about the relationships of Asparagales, see Petrosaviales. Note that H.-T. Li et al. (2019) place Petrosaviaceae (q.v.) as sister to Orchidaceae, and both contain mycoheterotrophic taxa, but this apparent relationship may well not hold up (Baker et al. 2021: see Seed Plant Tree).
The tree (below) of relationships within Asparagales is based largely on the analyses in Chase et al. (2000a) and Fay et al. (2000: successive weighting). These studies differ little in detail, although the analysis of Fay et al. (2000) hardly surprisingly had more nodes in the core Asparagales with strong support; they are consistent with relationships in Chinese Asparagales as detailed in Z.-D. Chen et al. (2016) and the relationships in McLay and Bayly (2016), although the focus of the latter was Asphodelaceae. For the [Amaryllidaceae + Agapanthaceae] clade, see Meerow et al. (2000b), and relationships between Aphyllanthaceae, Themidaceae and Hyacinthaceae might be better represented as trichotomy (see also S. Chen et al. 2013); these families are now subsumed in a broadly-drawn Amaryllidaceae and Asparagaceae respectively. The relationships in McPherson and Graham (2001) and D.-K. Kim et al. (2012) are largely congruent with those in the tree below, although their sampling is poorer and more geographically constrained. In some phylogenetic reconstructions of Hilu et al. (2003) Asparagales were paraphyletic, Orchidaceae being separate from the rest.
Understanding the relationship between Boryaceae and Orchidaceae is important Because it affects our ideas of diversification. Boryaceae have been placed as sister to Orchidaceae (e.g. Chase et al. 1995a; McPherson & Graham 2001), although with rather weak support. Janssen and Bremer (2004) found the relationships [[Boryaceae, Blandfordiaceae, etc.] [Orchidaceae [Ixoliriaceae [Tecophilaeaceae [Doryanthaceae + The Rest]]]]], while Orchidaceae were embedded in a Boryaceae-Hypoxidaceae clade (X.-X. Li & Zhou 2007), but again, with little support. In Wikström et al. (2001) Orchidaceae were sister to Hypoxidaceae, while Rudall (2003a: morphological data) also suggested that there was a close relationship between Hypoxidaceae and Orchidaceae in particular, and also between Boryaceae and Blandfordiaceae and Iridaceae and Doryanthaceae. Seberg et al. (2012) largely recovered the topology found by earlier workers; mitochondrial data provided little support for the backbone of the tree and mitochondrial and chloroplast data agreed only after removing edited mitochondrial sites.
Most more recent work suggests that Orchidaceae are sister to all other Asparagales (e.g. 76% bootstrap support in Graham et al. 2006; about the same in Givnish et al. 2006b; stronger [96-99%] in Pires et al. 2006: good sampling, seven genes from two compartments; Chase et al. 2006; S. Chen et al. 2013). There was more or less strong support for the [Boryaceae, Blandfordiaceae et al.] clade in these analyses. All in all, the topology [Orchidaceae [[astelioids] [all other Asparagales]]], seems the best hypothesis. This affects the characterisation of Asparagales, since some characters previously considered to refer to Asparagales as a whole move to the next node up (c.f. versions 6 and younger of this site; there Orchidaceae were not sister to the rest of the order). However, if recent suggestions that Petrosaviaceae are sister to Orchidaceae (H.-T. Li et al. 2019) are confirmed, the positions of these characters will have to be rethought.
Within the astelioids, a clade [Asteliaceae [Lanariaceae + Hypoxidaceae]] was recovered by S. Chen et al. (2013), while in Chase et al. (2006) Boryaceae were placed immediately above the Blandfordiaceae et al. clade, albeit with very little support. For some reason I had earlier had a grouping [Lanariaceae [Asteliaceae + Hypoxidaceae]], but this has been corrected (see also H.-T. Li et al. 2019). The clade [[Ixoliriaceae + Tecophilaeaceae] [Doryanthaceae [Iridaceae [Xeronemataceae + The Rest]]]] is strongly supported in analyses using data from four plastid genes (Fay et al. 2000; see also Chase et al. 2000a; Soltis et al. 2007a), but no morphological characters have yet been found for it. The positions of [Ixoliriaceae + Tecophilaeaceae] and Doryanthaceae are reversed in Kim et al. (2011) and in Fig. 2 in S. Chen et al. (2013), although in their Fig. 3 the three families are shown forming a clade [Doryanthaceae [Ixoliriaceae + Tecophilaeaceae]], and they do have a few features in common. Givnish et al. (2018b) found that the clade [Doryanthaceae [Iridaceeae ... Asparagaceae]] had rather poor support.
Classification. There have been suggestions that Orchidaceae should be placed in their own order, either because of their age and/or diversity and morphology (e.g. Eguchi & Tamura 2016). Quite extensive changes in names and group circumscriptions in the order have made for a less than an ideal situation, but one still hopes for stability. However, there are clearly problems in the acceptance of the APG classification in the Asphodelaceae-Amaryllidaceae-Asparagaceae area (Nyffeler & Eggli 2010b, 2020; Nordal & Sletten-Bjorå 2016), and with the Asparagaceae s.l. in particular one can see what the issues are - nothing characterises that clade.
Previous Relationships. Dahlgren et al. (1985) took important steps in reorganizing the relationships of the "lily-like monocots". They recognized two groups, Asparagales and Liliales, which were separable by features including patterning of the tepals and absence of phytomelan, both features of their Liliales. However, they still included Iridaceae and Orchidaceae in Liliales.
Synonymy: Asparagineae J. Presl, Asphodelineae Thorne & Reveal, Hyacinthineae Link, Iridineae Engler, Scillineae J. Presl - Agavales Hutchinson, Alliales Berchtold & J. Presl, Amaryllidales Link, Apostasiales Martius, Asphodelales Doweld, Asteliales Dumortier, Gilliesiales Martius, Hypoxidales Martius, Iridales Rafinesque, Ixiales Lindley, Narcissales Dumortier, Orchidales Rafinesque, Tecophilaeales Reveal, Xanthorrhoeales Reveal & Doweld
ORCHIDACEAE Jussieu, nom. cons. - Back to Asparagales
Mycorrhizal herbs; flavone C-glycosides, flavonols +, chelidonic acid?; roots with velamen + exodermis; stomata frequently tetracytic; leaf vascular bundle sheaths with fibres, (also fibre bundles in leaves); flowers rather weakly monosymmetric, median outer T adaxial [flowers described here as if upside-down]; T free, lateral outer T first to develop, median member the last, median [abaxial] inner T differentiated [= labellum]; A 3, [median of outer whorl and laterals of inner whorl], basally adnate to style; endothecial thickenings annular; tapetal cells uninucleate; pollen with elastoviscin; septal nectaries 0, placentation intrusive parietal, placentae bilobed, style solid [?all], stigmas commissural, wet; ovules ca 1500+/carpel, parietal tissue none, funicle not vascularized; fruit dehiscing laterally, loculicidal, interplacental areas separating, T deciduous in fruit; seeds minute; testa 1-layered, air space between testa and embryo, endosperm barely developing, none at maturity, embryo minute, undifferentiated [radicle 0], suspensor often haustorial (and branched); x = 10 (?11), nuclear genome [1 C] (0.182-)3.529(-68.513) pg; whole genome duplication, ca 270 bp transfer from fungal to orchid mitogenome; seedling forming protocorm, mycoheterotrophic.
Ca 880[list, to tribes]/26,000 - five subfamilies below. World-wide. [Photo - Flower]
Age. Crown group Orchidaceae have been dated to ca 111 Ma (Janssen & Bremer 2004) or (121-)93.7(-75) Ma (Chomicki et al. 2014c; see also X.-G. Xiang et al. 2017). The estimates of Ramírez et al. (2007, see esp. Supplementary Table) are somewhat younger at (90-)84-76(-72)Ma but (105-)80(-56) Ma when recalculated by Gustafsson et al. (2010). Other crown group estimates include (105-)80-77(-56) Ma (Gustafsson et al. 2010; Leopardi-Verde et al. 2016: similar, less spread; G.-Q. Zhang et al. 2017: ca 81 Ma, wider spread), while ages in Givnish et al. (2015, 2016a), at (99.5-)90(79.7) Ma (and with a ca 20 Ma stem) and Bouetard et al. (2010) were slightly older, and the youngest, (82-)68(-54) or ca 51.6 Ma, are those in S. Chen et al. (2013) and (85.5-)68.9-)55.6) Ma in Y.-K. Kim et al. (2019). Ages in Serna-Sánchez et al. 2021) are ca 88.2 (strict clock) or ca 89.8 Ma (relaxed clock), phylogenetic fuses ca 35.4 and 23.9 Ma respectively. Finally, although Janssen and Bremer (2004) did not recover Orchidaceae as sister to the rest of Asparagales, its stem-group origin was near the beginning of divergence within the order and was ca 119 Ma.
1. Apostasioideae Horaninov
Roots tuberous, tubers with irregular papillae; ?chemistry; root velamen uniseriate, pith with scattered vascular bundles, vessel elements often with simple perforation plates; (vessels in stem +); stegmata with conical SiO2 bodies; leaves spiral, vernation plicate; flowers (not resupinate, ± polysymmetric - Apostasia); T apiculate, carinate [prominent midrib], plain coloured, (labellum 0 - Apostasia), develop from a ring primordium, lateral members of inner whorl develop first; (A 2, staminode +/0 - Apostasia); pollen surface reticulate, colpus operculate; placentae meeting, with central cavity, stigma papillate, lobes spreading; micropyle bistomal; (embryo sac bisporic, the spores chalazal, 8-celled [Allium type] - Neuwiedia); fruits (baccate), (dehiscing irregularly); seeds dark in colour, ?endotestal, exotesta with cuticular layer, cells isodiametric, lignified [Neuwiedia], outer periclinal walls collapsing; n = 24.
2/15. Sri Lanka, N.E. India to N.E. Australia, Japan (map: from Pridgeon et al. 1999).
Age. Estimates of the age of crown-group Apostasioideae are (54-)49-45(-41) Ma (Ramírez et al. 2007), or (66-)43(-23), (61-)41(-23) Ma (Gustafsson et al. 2010) and ca 29.1 Ma (Y.-K. Kim et al. 2019). Ages in Serna-Sánchez et al. 2021) are ca 39.8 (strict clock) or ca 36.4 Ma (relaxed clock), phylogenetic fuses ca 48.4 and 53.4 Ma respectively.
Synonymy: Apostasiaceae Lindley, Neuwiediaceae Reveal & Hoogland
[Vanilloideae [Cypripedioideae [Orchidoideae + Epidendroideae]]]: C-glycosyl flavones, (saponins), 6-hydroxy flavonols +; vessel elements with scalariform perforation plates; leaves two-ranked; flowers strongly monosymmetric; ?abaxial outer tepal develops after inner whorl, labellum strongly differentiated, develops before other members of the inner whorl; the style and A almost completely congenitally fused [column, = gynostemium], anthers to 2x as broad as long; pollen sticky; median G initiated first, initially much larger, placentation parietal, hairs/papillae on inside of carpel wall, stigma asymmetric [lateral lobes, + part median lobe]; ovules not fully developed at pollination, (embryo sac 6-nucleate); fertilization may take some months; exotestal cells ± elongated; radicle 0.
Age. The age of this node is around 71 Ma (Gustafsson et al. 2010), (92.9-)84(-74.4) Ma (Givnish et al. 2015, 2016a) and (73.7-)59.3(-44.7) Ma (Y.-K. Kim et al. 2019). Ages in Serna-Sánchez et al. 2021) are ca 85 (strict clock) or ca 89.8 Ma (relaxed clock).
2. Vanilloideae Szlachetko
Plant (monopodial - Vanilla), often viny, (echlorophyllous, mycoheterotrophic, associated with ECM fungi); (lignin with catechyl units - Vanilla); velamen uniseriate; plant glabrous; stomata notably variable; (leaf blade venation reticulate); (calyculus +); T often carinate, (margins of labellum fused with column - some Vanilleae); A 1 [= median [abaxial] member of outer whorl], staminodes 2 [= lateral members of inner whorl], anther incumbent [bent forward] by massive expansion of the apical column/connective; "pollinia" +, soft [not highly organized], viscidium 0; pollen inaperturate[?], (polyporate), (in tetrads), smooth or not; (placentation axile), rostellum [ridge, part of median stigmatic lobe] +; (T persistent in fruit), (fruit baccate); seeds often relatively large, (winged), (spherical, crustose, [testal - outer parietal wall well developed], tegmen persisting), (exotesta with cuticular layer); endosperm 0 or to 16-nucleate; n = 9, 10, 12, 14-16, 18, etc..
14/245: Vanilla (105), Cleistes (64). Pantropical, esp. Asia, inc. Australia, some N. America (map: from Pridgeon et al. 2003).
Age. Crown group Vanilloideae are (76-)71-65(-61) Ma (Ramírez et al. 2007), or (79-)58, 57(-43) Ma as recalculated by Gustafsson et al. (2010), while ca 71 Ma is the estimate in Bouetard et al. (2010) and around abour 77 Ma in Givnish et al. (2016a). Ages in Serna-Sánchez et al. 2021) are ca 81.0 (strict clock) or ca 67.7 Ma (relaxed clock), phylogenetic fuses ca 4.0 and 12.7 Ma respectively.
Synonymy: Vanillaceae Lindley
[Cypripedioideae [Orchidoideae + Epidendroideae]]: (velamen multiseriate), tilosomes +; exotesta lacking cuticular layer.
Age. The age of this clade is estimated at only 37-26 Ma by Wikström et al. (2001), (69-)48, 42(-23) Ma by Bell et al. (2010), around 69-68 Ma by Gustafsson et al. (2010), (87.4-)76(-64.6)Ma by Givnish et al. (2015, 2016a) and (66.1-)52.9(-42.9) by Y.-K. Kim et al. (2019). Ages in Serna-Sánchez et al. 2021) are ca 70.1 (strict clock) or ca 76.9 Ma (relaxed clock).
3. Cypripedioideae Kosteletzky
Plant (epiphytic, epilithic); root with persistent hairs, (pith 0 - some Cypripedium); stem bundles amphivasal; stomata anomocytic - Cypripedium; leaf blade vernation (plicateconduplicate); (flowers not resupinate [when single]); outer T valvate/open, 2 abaxial T of outer whorl connate, labellum saccate; A 2 [= lateral members of inner whorl], (pollinia +), staminode single, conspicuous [= median member of outer whorl]; tapetal cells binucleate; microsporogenesis successive?; pollen sulcate, ± smooth [psilate], (foveolate), (in tetrads), sticky or not; (placentae meeting, with central cavity), stigma lobes spreading, (papillate), median lobe largest; (micropyle bistomal); embryo sac bisporic [chalazal dyad], eight-celled [Allium-type]; (T persistent in fruit); (outer periclinal wall of testa sclerified - Selenipedium); n = 9 or more; (chloroplast ndh genes not functional).
5/170: Paphiopedilum (86), Cypripedium (51). Mostly (warm) temperate N. Hemisphere, East Malesia and tropical South America (S. India) (map: from Hultén 1958; Pridgeon et al. 1999). [Photo - Flower]
Age. Crown group Cypripedioideae are (54-)49-44(-39)/(66-)43-41(-23) Ma (Ramírez et al. 2007), but recalculated as (50-)33, 31(-17) Ma by Gustafsson et al. (2010), while from Fig. 1 in Givnish et al. (2016a) their age is around 63 Ma and it is ca 68 Ma in Guo et al. (2012: Fig. 4, several younger ages also suggested) but in Y.-K. Kim et al. (2019) it is only ca 27.5 Ma... Ages in Serna-Sánchez et al. 2021) are ca 31.5 (strict clock) or ca 38.5 Ma (relaxed clock), phylogenetic fuses ca 38.5 and 31.5 Ma respectively.
Synonymy: Cypripediaceae Lindley
[Orchidoideae + Epidendroideae]: plant (echlorophyllous, mycoheterotrophic, associated with ECM fungi); leaves withering on the plant; flowers resupinate [ovary twisted]; floral primordium transversely elliptic-oval; labellum initiated first; A 1 [= median [abaxial] member of outer whorl], sporangia 2 [?level], (staminodes 2 [from outer whorl]); [tetrads tetrahedral]; pollinia +, attached to sticky viscidium, pollinium/pollinarium stalk variously formed; pollen in tetrads (monads), inaperturate, (porate or ulcerate); median [adaxial] carpel developed before the others, rostellum + [ridge, part of median stigmatic lobe, viscidium is also part of it]; T persistent in fruit; phytomelan 0, tegmen not persisting; endosperm not developing at all; n = 9 or more [19 common].
Age. The age of this node is estimated to be around 59-51 Ma (Gustafsson et al. 2010), (73.7-)64(-54.8) Ma (Givnish et al. 2015, 2016a), (72.5-)61.5(-51.7) Ma (Leopardi-Verde et al. 2016) or (55.8-)44.7(-36.2) Ma (Y.-K. Kim et al. 2019). Ages in Serna-Sánchez et al. (2021) are ca 63.2 (strict clock) or ca 68.4 Ma (relaxed clock).
4. Orchidoideae Eaton
Root tubers +/0 (fleshy rhizomes +); (glucomannans +); (amyloplasts with numerous minute starch grains [= spiranthosomes]); (tilosomes 0); sclerenchyma in leaf [as fibre bundles or associated with vascular bundles] and stem rare; stomata anomocytic; leaves (spiral), soft, herbaceous; anther erect (incumbent), apex acute, staminodes of inner whorl reduced; pollinia soft/sectile, (hamulus + [= pollinium stalk, from recurved apical part of rostellum]), (caudicles + [= pollinium stalk, from basal extension of pollinia]), pollen usu. intectate; n = 12-24 [x = 7?].
208/3,755: [CR = Cranichideae, DI = Diurideae, OR = Orchideae] Habenaria (OR: 840), Caladenia (DI: 270), Platanthera (OR: 136), Pterostylis (CR: 215), Disa (OR: 182), Cynorkis (OR: 156), Microchilus (CR: 145), Corybas (DI: 140), Prasophyllum (DI: 131), Thelymitra (DI: 110), Peristylus (OR: 105), Satyrium (OR: 86), Disperis (OR: 78), Cyclopogon (CR: 83), Pelexia (CR: 77), Zeuxine (CR: 74), Diuris (DI: 70), Goodyera (CRA: 70), Ponerorchis (OR: 55), Cheirostylis (CR: 53), Herminium (OR: 49), Sarcoglottis (CR: 48), Vrydagzynea (CR: 43). World-wide, esp. temperate (map: from Pridgeon et al. 2001, 2003; distribution in N. Asia and N. North America unclear).
Age. Crown group Orchidoideae are (63-)58, 52(-48) Ma (Ramírez et al. 2007), or, as recalculated by Gustafsson et al. (2010), (67-)50(-34) Ma and (64-)53(-42) Ma. Ages in Serna-Sánchez et al. (2021) are ca 57.8 (strict clock) or ca 60.0 Ma (relaxed clock), phylogenetic fuses ca 5.4 and 8.4 Ma respectively.
[Cranichideae + Diurideae] ?. Ages in Serna-Sánchez et al. (2021) are ca 55.8 (strict clock) or ca 53.2 Ma (relaxed clock).
Cranichideae: Pterostylis (215), Microchilus (145), Cyclopogon (83), Pelexia (77), Zeuxine (74), Goodyera (70), Cheirostylis (53), Sarcoglottis (48), Vrydagzynea (43). Ages in Serna-Sánchez et al. (2021) are ca 46.0 (strict clock) or ca 41.6 Ma (relaxed clock), phylogenetic fuses ca 9.8 and 11.6 Ma respectively.
Diurideae (Endlicher) Meisner: Caladenia (270), Corybas (140), Prasophyllum (131), Thelymitra (110), Diuris (70). Ages in Serna-Sáchez et al. (2021) are ca 54.4 (strict clock) or ca 40.9 Ma (relaxed clock), phylogenetic fuses ca 1.4 and 12.4 Ma respectively.
Codonorchideae P. J. Cribb: 1/2. S.E. Brazil, E. Argentina and Chile, Falkland Islands.
Orchideae: Habenaria (840), Platanthera (136), Disa (182), Cynorkis (156),Peristylus (105), Satyrium (86), Disperis (78), Ponerorchis (55), Herminium (49). Ages in Serna-Sánchez et al. (2021) are ca 38.5 (strict clock) or ca 41.1 Ma (relaxed clock), phylogenetic fuses ca 15.3 and 13.2 Ma respectively.
Synonymy: Neottiaceae Horaninow, Limodoraceae Horaninow, Liparidaceae Vines, Ophrydaceae Vines
5. Epidendroideae Kosteletzky
Epiphytes common, plant fleshy [stems, leaves]; growth (monopodial - Vandeae); (pyrrolizidine alkaloids + [esp. phalaenopsines]); roots (with pneumathodes), (the main photosynthetic organs of the plant - some Vandeae), (velamen 0); stegmata with conical/(spherical) SiO2 bodies/0; bicellular mucilage-secreting floral hairs +; stomata often paracytic; leaves (unifacial, terete/isobifacial), (articulated and deciduous above sheathing base), vernation conduplicate (plicate); anther incumbent [bent forwards], (strongly convex), with beak, operculate; pollen (semitectate); endothecial thickenings often other than annular; pollinia hard/(soft/sectile), 2-12, clavate, with a waxy surface; (tegulum + [= pollinium strap formed from epidermis (and subjacent cell layers) of rostellum] - vandoids); (inside of carpel wall with hairs); (cotyledon visible); n = 5+; (chloroplast ndh genes not functional); ca 8 kbp transfer from fungal to orchid mitogenome.
650/21,800 (14 tribes: AR = Arethuseae, CY = Cymbidieae, EP = Epidendreae, MA = Malaxideae, NEO = Neottieae, PO = Podochileae, SO = Sobralieae, VA = Vandeae): Bulbophyllum (MA: 1,870-?2,200), Dendrobium (MA: 1,700), Epidendrum (EP: 1,425), Lepanthes (EP: >1,200), Stelis (EP: 1,120), Maxillaria (CY: 665), Masdevallia (EP: 625), Pleurothallis (EP: 555), Liparis (MA: 320-430), Oberonia (MA: 325), Oncidium (CY: 315), Dendrochilum (AR: 280), Crepidium (MA: 260), Eria (PO: 240), Polystachya (VA: 240), Calanthe (CO: 220), Angraecum (VA: 220), Phreatia (PO: 215), Pinalia (PO: 210), Telipogon (CY: 205), Acianthera (EP: 200), Coelogyne (AR: 200), Eulophia (CY: 200), Malaxis (MA: 185), Taeniophyllum (VA: 190), Octomeria (EP: 160), Appendicula (PO: 150), Catasetum (CY: 180), Thrixspermum (VA: 180), Encyclia (EP: 170), Anathallis (EP: 155), Ceratostylis (PO: 150), Sobralia (SO: 150), Cyrtochilum (CY: 140), Pabstiella (EP: 140), Dracula (EP: 135), Glomera (AR: 130), Anathalis (EP: 120), Dichaea (CY: 120), Gomesia (CY: 120), Prosthecea (EP: 120), Cattleya (EP: 115), Elleanthus (SO: 110), Platystele (EP: 110), Trichosalpinx (EP: 110), Agrostophyllum (EP: 100), Gastrodia (GA: 100), Specklinia (EP: 100), Brachionidium (EP: 80), Cleisostoma (VA: 80), Comparettia (CY: 80), Mormodes (CY: 80), Trichotosia (PO: 80), Gongora (CY: 75), Vanda (VA: 75), Andinia (EP: 70), Campylocentrum (VA: 70), Cymbidium (CY: 70), Kefersteinia (CY: 70), Phalaenopsis (VA: 70), Scaphyglottis (CY: 70), Trichoglottis (VA: 70), Trichocentrum (CY: 70), Nervilia (NER: 67), Neottia (NEO: 65), Brassia (CY: 64), Podochilus (PO: 62), Coryanthes (CY: 60), Cylindrolobus (PO: 60), Kefersteinia (60), Stanhopea (CY: 60), Sophronitis (60), Aerangis (VA: 58), Gastrochilus (VA: 56), Notylia (CY: 56), Dryadella (EP: 55), Muscarella (EP: 55), Ornithidium (MA: 55), Ornithocephalus (CY: 55), Porroglossum (EP: 53), Restrepia (EP: 53), Octarrhena (PO: 52), Fernandezia (CY: 51), Epipactis (NEO: 50), Myoxanthus (EP: 50), Scaphosepalum (EP: 50). More or less world-wide, but most diverse in the tropics; rather poorly developed in Australia (map: from Pridgeon et al. 2005).
Age. Crown group Epidendroideae are estimated to be (67-)59, 51(-44) Ma (Ramírez et al. 2007), or recalculated as (62-)49, 44(-29) Ma (Gustafsson et al. 2010), ca 48 Ma (Givnish et al. 2016a) and (58.9-)48.6(-39.1) Ma (Leopardi-Verde et al. 2016); other estimates include (115-)97.7(-83) Ma (Sosa et al. 2016, q.v. for discussion) and (49.5-)39.8(-32.0) Ma (Y.-K. Kim et al. 2019). Ages in Serna-Sánchez et al. (2021) are ca 44.5 (strict clock) or ca 60.2 Ma (relaxed clock), phylogenetic fuses ca 18.7 and 8.2 Ma respectively.
Succinanthera baltica, consisting of pollinaria attached to a fungus gnat found in Baltic amber ca 55-45 Ma, has been placed in Epidendroideae, perhaps belonging to a basal clade (Poinar & Rasmussen 2017).
[Neottieae [Sobralieae [Arethuseae [Malaxideae [Collabieae [Vandeae [Cymbidieae + Epidendreae]]]]]]]
Neottieae: Ages in Serna-Sánchez et al. (2021) are ca 35.6 (strict clock) or ca 56.3 Ma (relaxed clock), phylogenetic fuses ca 8.9 and 4.0 Ma respectively.
Sobralieae: Ages in Serna-Sánchez et al. (2021) are ca 7.7 (strict clock) or ca 11.5 Ma (relaxed clock), phylogenetic fuses ca 33.1 and 41.8 Ma respectively.
[Arethuseae [Malaxideae [Collabieae [Vandeae [Cymbidieae + Epidendreae]]]]]: epiphytes common, with water-storing hypodermis.
Arethuseae: Ages in Serna-Sánchez et al. (2021) are ca 19.8 (strict clock) or ca 22.5 Ma (relaxed clock), phylogenetic fuses ca 16.9 and 23.6 Ma respectively.
Malaxideae: Ages in Serna-Sánchez et al. (2021) are ca 33.7 (strict clock) or ca 37.0 Ma (relaxed clock), phylogenetic fuses ca 2.2 and 7.9 Ma respectively.
Collabieae: Ages in Serna-Sánchez et al. (2021) are ca 17.3 (strict clock) or ca 22.5 Ma (relaxed clock), phylogenetic fuses ca 14.6 and 13.5 Ma respectively.
[Vandeae [Cymbidieae + Epidendreae]]
Age. This clade is (31.1-)25.3(-21.2) Ma (Y.-K. Kim et al. 2019).
Epidendreae: Ages in Serna-Sánchez et al. (2021) are ca 32.2 (strict clock) or ca 35.5 Ma (relaxed clock), phylogenetic fuses ca 2.6 and 5.2 Ma respectively.
Vandeae: Ages in Serna-Sánchez et al. (2021) are ca 25.6 (strict clock) or ca 30.8 Ma (relaxed clock), phylogenetic fuses ca 8.9 and 9.3 Ma respectively.
Cymbidieae: Ages in Serna-Sánchez et al. (2021) are ca 31.6 (strict clock) or ca 35.4 Ma (relaxed clock), phylogenetic fuses ca 2.9 and 4.7 Ma respectively.obieae and Vandeae is estimated to be ca 43 Ma (G.-Q. Zhang et al. 2017).
Synonymy: Pycnanthaceae Ravenna
Evolution: Divergence & Distribution. Neither Mycophoris, an orchid seed in Dominican amber at least 20-15 Ma, and its associated fungus (Poinar 2016a) are likely to have been correctly identified (Selosse et al. 2017b). However, Iles et al. (2015) give dates for three fossils reliably placed within Orchidaceae and Poinar (2016b) described pollinaria attached to beetles and stingless bees in Dominican and Mexican amber some Ma respectively.
See Pérez-Escobar et al. (2017a: Fig. S7-S9) for ages, the focus on Epidendreae and Pleurothallidinae, also Fischer et al. (2007: Bulbophyllum), Sosa et al. (2016: Epidendreae), X.-G. Xiang et al. (2017) and H.-T. Li et al. (2019), both Dendrobium, Andriananjamanantsoa et al. (2016), Pessoa et al. (2018) and Faminhão et al. (2021), all Angraecum and relatives, etc.. Serna-Sánchez et al. (2021) suggest a number of ages for major clades in the family, but these differ, and sometimes quite substantially, depending on whether strict or relaxed clock methods are being used, and this also applies to the stem branch lengths (= phylogenetic fuses) of these clades. Thus 13/17 crown group ages are older if relaxed clock methods are used, while 11/17 stem-group ages are older (the clades with younger ages differ in the two methods); as an example, strict clock estimates of the age of Diurideae are ca 54.4 Ma for the crown group and ca 1.4 Ma for the stem group, while with a relaxed clock the comparable ages are ca 40.9 and 12.4 Ma respectively (Serna-Sánchez et al. 2021); evolutionary stories that depend on these ages will be different.
Diversification may have increased at this node around (108.8-)73.1(-59.7) Ma (Magallón et al. 2018) - but see below.
We still know rather little about the origin and biogeography of the family (see also Chase 2003). Givnish et al. (2016a) suggested that Orchidaceae originated in Australia ca 112 Ma and then spread via Antarctica to South America where Vanilloideae and Cypripedioideae originated by 64 Ma. Ramírez et al. (2007) also thought that the subfamilies had diverged by the end of the Cretaceous, ca 65 Ma (see also Givnish et al. 2015, 2016a), or perhaps slightly later in the early Palaeocene, and that orchid radiation has been a Caenozoic phenomenon; dates suggested by Gustafsson et al. (2010) are somewhat younger, major diversification perhaps occurring during the cooler period at the end of the Eocene and into the Oligocene rather than during the thermal maximum earlier in the Eocene (c.f. Ramírez et al. 2007).
Despite the minute size of orchid seeds, long distance dispersal (l.d.d.) seems not to be notably common in the family (c.f. Vollering et al. 2015), and orchid species may be narrowly distributed despite the wide distribution of some of their fungal associates (Davis et al. 2015; see also Weiß et al. 2016: Sebacinales-Serendipitaceae the fungi). Indeed, there can be surprisingly little genetic differentiation between orchid populations, despite the possibility for l.d.d. of the seeds and resultant founder effects (Phillips et al. 2012), perhaps because l.d.d. swamps potential geographic variation... However, epiphytic taxa in tropical mountains may show quite a bit of local genetic divergence (Givnish et al. 2015 for literature). Pérez-Escobar et al. (2017a, see also b) noted that the Andes seems not to have been much of a barrier to the dispersal of Cymbidieae and Pleurothallidineae whose diversification they were studying. There are a few cases where l.d.d. does seem to have been a factor. Givnish et al. (2016a) estimated that there had been around 73 l.d.d. events in his study of the family, even if the distributions of over 97% of orchid species are restricted to single continents. Bouetard et al. (2010) estimated that Vanilla started to diversify ca 34 Ma, at least three instances of l.d.d. being needed to explain its present distribution, while l.d.d. seems also to be quite common in Spiranthes with S. romanzoffiana occuring on both sides of the Atlantic, movement having been from west to east (Dueck et al. 2014 and refs). Kirby (2016) looked at possible l.d.d. in tropical American orchids. L.d.d. is a common way in which plants get to oceanic islands, and here the relatively low diversity of orchids compared to groups like Asteraceae (Lenzner et al. 2017), perhaps connected with the obligate association of germinating orchid seeds with fungi, but it at first sight does seem odd. That orchids arrived on Krakatau, Indonesia (Partomihardjo 2003), quite soon after its devastating eruption is of doubtful relevance since Krakatau is preeminently a continental island. Traxmandlová et al. (2017 and references) suggested that species richness of orchids on islands depended in considerable part on area and altitude, i.e. habitat diversity.
Diversification in the seven or eight tribes of the speciose core/advanced/upper Epidendroideae, largely epiphytic, began 37.9-30.8 Ma (Gravendeel et al. 2004; Givnish et al. 2015; see also Freudenstein & Chase 2015). Speciation may have increased in these clades, e.g. in Epidendroideae-Malaxidae-Dendrobiinae, partly because of the adoption of the epiphytic habit and movement into montane areas (Givnish et al. 2015), and because of changes in the rate of uplift of the Andes (Pérez-Escobar et al. 2017a). However, other apomorphies deeper in Orchidaceae, while having no obvious immediate effect on diversification, may have combined to affect diversification at these higher levels (Givnish et al. 2015: see also below). There are ca 8,450 neotropical species of Cymbidieae and Pleurothallidinae, mostly Andean. Clades of Cymbidieae, most diverse below 800 m, are largely derived from Amazonian lowland taxa (41-)34(-27) Ma (stem age), most diversification being after ca 25 Ma, while Pleurothallidinae are most diverse between 400 and 2200 m, clades largely being derived from lineages preadapted to cool conditions, comparable ages being (27-)20(-13) and ca 17 Ma (Pérez-Escobar et al. 2017a). On the other hand, in the largely terrestrial (a reversal) Epidendreae-Calypsoinae there is a decrease in the rate of speciation (Givnish et al. 2015, see also 2016a); see also Sosa et al. (2016) for another example of the derived terrestrial habit in Epidendreae.
Some major clades in Epidendroideae ae worth noting. In the largely Old World and very diverse Bulbophyllum the few (ca 60) New World species form a clade sister to the African taxa, the overall geographical pattern being [S. E. Asia [Madagascar [Africa [Africa + New World]]], and the genus may have initially evolved in Southeast Asia (Gravendeel et al. 2004; Smidt et al. 2011; esp. B. Gravendeel, E. de C. Smidt, G. Fischer & J. J. Vermuelen in Pridgeon et al. 2014), with some 500 species in New Guinea alone. Bulbophyllum is quite diverse on Africa-Madagascar, where the major epiphytic group are the angraecoid orchids (all told, some species). Diversification in these latter began in the Miocene (24.0-)17.6(-11.1) Ma; Faminhão et al. (2021) noted that there was some similarity in the patterns of diversification of the Angraecum group and Bulbophyllum. The Angraecum group is noted for its extensive dysploidy (but Bulbophyllum is not!) but this seems not to be correlated with its diversification, although there may be links between chromosome number change and features like leaflessness and rostellum structure (Faminhão et al. 2021). Diversification in the largely Indo-Malesian Dendrobium with its 1,500+ species is estimated to have begun (31.6-)28.2(-25.1) Ma (X.-G. Xiang et al. 2016) or (47.7-)37.4(-29.5) Ma (M.-H. Li et al. 2019: split between Asian and Australasian clades). Interestingly, Pedersen et al. (2020) found small monophyletic groups of Dendrochilum (280 spp.), mainly West Malesian, on the same mountain. Epidendrum and Lepanthes are both New World, and with 1,549 and 1,035 species respectively they are two of the five largest genera there (Ulloa Ulloa et al. 2017).
About half the 180 species of the tuberous Disa (Orchidoideae-Orchideae) are restricted to the Cape Floristic Region, and they moved into subalpine/grassy habitats where they often flower immediately after fires, a habit that has been dated to around 12.9 Ma; they also diversified on the Drakensbergs (Bytebeier et al. 2011, see also Linder 2003; Galley et al. 2007).
There are some 295 species of more or less echlorophyllous mycoheterotrophs (= holomycoheterotrophs) here in Orchidaceae, over half of all mycoheterotrophic species (ca 530 spp.: Jacquemyn & Merckx 2019), and they have evolved some 25-30 or more times (Molvray et al. 2000; Merckx & Freudenstein 2010; Freudenstein & Barrett 2010; Merckx et al. 2013c; Feng et al. 2016; Lam et al. 2018). It has been suggested that Aphyllorchis, all 30+ species of which are mycoheterotrophs, diverged from Cephalanthera ca 28 Ma, however, A. montana, the only species studied by Feng et al. (2016), showed signs of being a young mycoheterotroph, several of its photosynthesis genes being putatively functional (see also Barrett et al. 2018). For more on mycoheterotrophy, obligate or not, see below.
Gravendeel et al. (2004 and references; see also Peakall 2007) list the numerous hypotheses that have been advanced to explain the diversity of Orchidaceae, not all mutually exclusive. These include pollinator specialization, niche partitioning, habitat fragmentation, and wide dispersal of the seeds. A genome duplication shared by all orchids has been implicated in the evolution of many of the adaptive traits found in the family (Unruh et al. 2016), thus G.-Q. Zhang et al. (2017) thought that the unbranched aerial roots of epiphytic orchids with their velamen, the absence of endosperm, and labellum and pollinium evolution could all perhaps be linked to particular gains and losses in the orchid genome when compared with that of other monocots. Note that some of the distinctive features of the family seem to be biologically connected, for example, pollinia ensure the fertilization of numerous ovules, the minute seeds that result are usually devoid of endosperm or a differentiated embryo, and the obligate mycoheterotrophy of the young plant may compensate for the absence of seed reserves and undifferentiated embryo (Johnson & Edwards 2000 in part; Eriksson & Kainulainen 2011).
Endress (2016: comparison with Apocynaceae) looked at flowers of Orchidaceae emphasizing the development of synorganization/complexity; synorganization lays the foundation for the development of novel structures, although it could be argued (see also below") that within the highly speciose [Orchidoideae + Epidendroideae] there is little real floral novelty, just infinite variation on a theme. Monosymmetry of the flower in many, but not all orchids - and in Hypoxidaceae and Doryanthaceae - is evident even in the earliest primordia (Kurzweil & Kocyan 2002 and references); although the flowers are usually presented inverted in all subfamilies, resupination in the sense of twisted ovaries seems not to occcur in the three basal subfamilies (Koopowitz 2017). Recent work suggests that PROLIFERATION CELL FACTOR and CINCINNATI gene families are much duplicated and are involved in the development of monosymmetry of flowers here (Madrigal et al. 2017: comparison between Cattleya trianae and Hypoxis decumbens), unlike the situation in other monosymmetric flowers. However, in their analysis of the complex evolutionary hostory of the RADIALIS and DIVARICATA gene lineages, Madrigal et al. (2019) found a common gene regulatory network involved in the control of floral symmetry in monocots and core eudicots. In Orchidaceae there were complex patterns of gene duplication that differed between the two groups of genes. A few Orchidaceae have more or less polysymmetric flowers, and in Telipogon (Epidendroideae-Oncidiinae) a polysymmetric perianth becomes evident only late in development (Pabón-Mora & González 2008). Duttke et al. (2012) discuss the remarkable terata to be found in Neofinetia falcata (Vandeae: Aeridinae) that have been accumulated in Japan over the last 350 years. For floral development and the expression of B-, C- and D-class genes in particular in Dendrobium, see Y. Xu et al. (2006); genes of all three classes are expressed in the column. Hsu et al. (2015) suggest how labellum development might be controlled; there was gene duplication after divergence of the lipless Apostasioideae, while Madrigal et al. (2017) note that there was a large-scale duplication event prior to the divergence of Epidendroideae and Orchidoideae. The sequence of organ initiation varies considerably within the family (Pabón-Mora & González 2008). Thus Apostasioideae and Cypripedioideae have simultaneous initiation of members of the inner tepal whorl, the plesiomorphic condition for Asparagales (Kocyan & Endress 2001a); have Vanilloideae been studied? Rudall et al. (2013b) attempt to work out what some of the parts of orchid flowers "are". They suggest connections between the auricles, which often have raphides, with inner whorl anthers of Apostasioideae, and they show that the bursicle, which had also been thought to be of staminodial origin, develops from lateral lobes of the median carpel. The labellum, which in its lobing they describe as being analogous to a compound leaf, has three traces - two come from the lateral sepals or perhaps originally from stamens of the outer whorl (Rudall et al. 2013b).
Endress (2011a) thought that the inferior ovary in Asparagales might be a key innovation, although where this feature should be placed on the tree is unclear - perhaps here is indeed one place. The presence of pollinia is another feature that he mentioned; this is probably best placed as a synapomorphy of the [Orchidoideae + Epidendroideae] clade. Indeed, orchid diversity is most often attributed to the nature of the association of the plant with its pollinator, as is discussed below. For details on the distinctive pollinaria of many epiphytic Epidendroideae, see Freudenstein and Chase (2015), who noted that "vandoid" anthers may increase pollinator specifity and so promote diversification. Mosquera-Mosquera et al. (2019) suggest that the ancestor of Epidendroideae had a pollinarium with four granular pollinia, caudicle, tegulum and viscidium.
But as to which of all these features might indeed be key innovations, that is another matter. Overall, species richness in tropical orchids is highest in montane habitats, usually in the 1,000-2,000 m zone although in the 2,000-3,000 m zone in New Guinea (Vollering et al. 2015), and the orchids involved are largely epiphytic members of the core Epidendroideae (Givnish et al. 2015, 2016a; see also Kirby 2016). (Orchidaceae are only the third most diverse family in lowland Amazonia, behind Fabaceae and Rubiaceae - Cardoso et al. 2017.) For the link between habitat diversity and orchid species richness on the islands of the tropical southwest Pacific, see Keppel et al. (2016). Normally neither orchids nor pollinating insects are diverse on oceanic islands, but angraecoid orchids are surprisingly diverse on the Mascarene islands, of which Réunion in particular also has a diverse insect fauna (Micheneau et al. 2008). I return to the issue of the apparent species richness of Orchidaceae and what may cause it below.
Ecology & Physiology.
Fungi and Orchids.
The obligate association of orchids with mycorrhizal saprotrophic or ectomycorrhizal (ECM) fungi, mostly basidiomycetes (see also Bacterial/Fungal Associations below) is central to understanding the ecophysiology of the orchid plant (for reviews, see Rasmussen 2002; Imhoff 2009; Girlanda et al. 2011; Dearnalay et al. 2012, 2017; Oberwinkler et al. 2013; Hynson et al. 2013; Rasmussen et al. 2015; S. Zhang et al. 2018; Jacquemyn & Merckx 2019). The embryo is usually undifferentiated, and although Arditti (1967) suggested that a cotyledon was recognizable in the embryos of a few species, the species he mentioned are not basal in the tree. The sometimes rather protracted obligate and at least initially echlorophyllous subterranean mycoheterotrophic phase of the young plant compensates for the absence of reserves in the minute seeds; in all species, the very young plant depends on its fungal associates for nutrients. This plant-fungus association results in the formation of a protocorm (Peterson et al. 1998) which may have a very distinctive morphology; the protocorm is a tuberous mass that basically consists of hypocotyl + plumule, and although it lacks roots, it may have tufts of root hairs (Weber 1981; Whigham et al. 2008; Bustam et al. 2014), and these root hairs ("rhizoids") are sometimes described as being branched (Rasmussen ?1999). The fungal hyphae form pelotons, complex coils of hyphae, inside the host plant cells, and these may be digested by the host. This association with fungi is essential for the establishment of the orchid seedling, and it does not appear to be antagonistic (Rasmussen 1995; Johnson & Edwards 2000 in part; Eriksson & Kainulainen 2011; Leake & Cameron 2012; Perotto et al. 2014; Rasmussen & Rasmussen 2014).
Details of fungus-orchid associations in Apostasioideae were until recently unclear. However, the ECM basidiomycete Tulasnella, a genus also found in Cypripedium, etc., other fungi are in Ceratobasidiaceae (Kristiansen et al. 2001, 2004: Neuwiedia; see also Roche et al. 2010). Apostasia is associated with Ceratobasidiaceae (Yukawa et al. 2009), and they are found in the stomatiferous root tubercules that occur there (but not in Neuwiedia). The stomata are permanently open, the tubercles lack a velamen and exodermis and may make the plant better able to deal with the wet conditions in which it may grow (Stern & Warcup 1994, q.v. for other distinctive anatomical features of these tubercles, inc. a stele that is 3-6-arch rather than 18-34-arch). Perhaps surprisingly, it has recently been found that C, and perhaps aLso N, moves from Ceratobasidium to A. nipponica, i.e. the latter is a partial mycoheterotroph (Suetsugu & Matsubayashi 2020).
Light commonly inhibits germination, even in epiphytic species (Rasmussen et al. 2015), and although there the protocorms are chlorophyllous (as are those of some terrestrial species), yet an association with a fungus is still needed if the young orchid is to survive (Hynson et al. 2013). In vitro experiments suggest that seed germination in at least some orchids, especially those from oligotrophic habitats, is suppressed by nitrate (and the growth of the adult plant can be negatively affected), perhaps associated with the preference of orchids for organic nitrogen (Figura et al. 2019 and references), and this in turn is likely to be linked to their association with fungi. A few orchids can germinate in the absence of a fungus, and in vitro germination of several terrestrial Australian orchids using variously doctored "asymbiotic" media could be as effective using the standard "symbiotic" medium (Bustam et al. 2014).
Which came first, the dust seeds or the mycoheterotrophic association? This is a chicken-or-egg question, although Rasmussen and Rasmussen (2014) suggest that a developing association with ECM fungi was the spur. Sugars and nitrogen, the latter predominantly as nitrogen-rich amino acids, move from the fungus to the orchid (Zimmer et al. 2007; Kuga et al. 2014; Focha et al. 2016). Orchid fungi that are saprotrophic can break down cellulose, but not lignin, and nutrients, including sugars (c.f. ericoid mycorrhizae here), ultimately moving into the orchid come from these saprotrophic activities, although their plant cell wall degrading enzymes may also be involved in penetrating the cell walls of the orchid (Dearnaley et al. 2012; Kohler et al. 2015; Teixeira da Silva et al. 2015 for references). The number of copies of carbohydrate-active enzymes and proteins with a cellulos-binding domain in these fungi was as high as in white-rot fungi, and higher than in brown-rot fungi (Kohler et al. 2015). In orchid—mycoheterotroph associations nutrients move to the orchid by tolypophagy or ptyophagy. In the former nutrients move from the fungal pelotons inside the cell to the orchid; groups of collapsed hyphae remain, or the hyphae lyse. In ptyophagy breakdown affects both hyphae and orchid tissue (see Rasmussen 2002; Rasmussen & Rasmussen 2014). Overall, Tulasnella (Cantharellales, a basidiomycete) is prominent in both terrestrial and epiphytic orchids (Oberwinkler et al. 2017), and Sebacina, Ceratobasidium and Atractiellomycetes somewhat less so (Kottke & Kovács 2013; see also Sieber & Grünig 2013 for fungal root endophytes).
Some kind of fungal association is also pervasive in adult orchids, explaining why orchid-type mycorrhizae are found in 9% of all flowering plants (Brundrett 2009; Brundrett & Tedersoo 2018); the part of the plant that hosts the fungus can vary (Ramsay et al. 1986). Tulasnella is associated with a number of adult orchids, these are (largely) autotrophic (Summer et al. 2012; Ogura-Tsujita et al. 2012), fixing all their own C. However, at least some orchids are mixotrophic/partly mycoheterotrophic, obtaining some C from their own photosynthetic activities and some from their fungal associate (and perhaps other nutrients move, too), whether the fungus is parasitic on other plants (e.g. Armillaria), saprotrophic or mycorrhizal (e.g. Rasmussen 2002: Table 1; Hynson et al. 2013). Suetsugu et al. (2020a) established that C from decaying plant material moved to the orchid via saprotrophic fungi by finding 14C spikes from atomic bomb tests of the mid twentieth century in th orchid. Mixotrophy may be an adaptation to the low-light conditions of the forest floor (Roy et al. 2009 and references), as with Paris type AM associations, where the C in the plant at least sometimes has two sources (Giesemann et al. 2019). Plants of two species of Cephalanthera acquired ca half as much fungus-derived C under low-light conditions compared with fully mycoheterotrophic species, but much less than that as light increased, indeed, they became almost completely autotrophic under high light conditions (Preiss et al. 2010). Indirect associations with trees via ECM orchid associates are well known (e.g. Bidartondo & Read 2008; see also Bidartondo et al. 2004), and there can be bi- or unidirectional movement of C and nitrogen between chlorophyllous orchids and their fungi (e.g. Bidartondo et al. 2004; Cameron et al. 2008a, esp. 2008b; Hynson et al. 2009a, 2013). Recent work suggests that mixotrophy is very widespread (Selosse et al. 2017a for a review; Lallemand et al. 2018); it occurs in orchids associated with "Rhizoctonia", for which, see below (Gebauer et al. 2016) with up to 20% of the C needs of the plant coming from the fungus (Schweiger et al. 2018), even in orchids growing in high-light conditions in meadows (Schiebold et al. 2017). Interestingly, photosynthesates of the mixotrophic orchids themselves do not move into the perennating underground parts (D. L. Taylor et al. 2002), rather, C, etc., in these latter comes from the associated fungus, which in turn for the most part does not supply the above-ground parts of the plant. However, Cameron et al. (2008a, b) found that C moved from Goodyera repens to its associated fungus Ceratobasidium cornigerum, which is not an ECM fungus, while in some orchids C in the young above-ground shoots in the spring may also come from the fungus (Gonneau et al. 2014; Lallemand et al. 2018); the relationship between plant and ECM fungus in the protocorm and in the adult plant's underground parts are quite similar. All told, these compartmentalizations are unlike the situation in other mycorrhizal associations (but see some AM associations), and details of the movement of C and N between plant and fungus are complicated (see also Gebauer & Meyer 2003; Liebel et al. 2010). In a number of hetero-/mixotrophic orchids shoots do not appear above ground every year, the phenomenon of vegetative dormancy (Shefferson 2003, 2018; Reintal et al. 2010), the record apparently being 18 year's dormancy in Epipactis helleborine, and small plants may continue to grow during this period, perhaps because of their fungal associations, although in larger plants there is generally a cost to the plant (Hurskainen et al. 2018).
There have been around 25, perhaps over 30, separate transitions to full/obligate mycoheterotrophy in Orchidaceae, and these mycoheterotrophs are most common in ground-dwelling Epidendroideae, where about 1 in 10 species is a mycoheterotroph (Freudenstein & Barrett 2010; Merckx et al. 2013b); the plants usually grow in shady conditions. Fully mycoheterotrophic orchids lack chlorophyll and are totally dependent on the fungus for all carbon (and nitrogen) (e.g. Dearnalay et al. 2012; Hynson et al. 2013). As might be expected, the adoption of full mycoheterotrophy may be irreversible (Hynson et al. 2013), however, mycoheterotrophic and leafy taxa of Cymbidium can hybridize (C. macrorhizon x C. ensifolium: Ogura-Tsujita et al. 2014), and mixotrophy may reverse to autotrophy (Lallemand et al. 2019). Eriksson and Kainulainen (2011) and Merckx et al. (2013c) discuss the ecological drivers of the evolution of mycoheterotrophy, and Simard et al. (2012 and references) for fungal specificity, with a reminder that there is a continuum between autotrophs and echlorophyllous obligate mycoheterotrophs (see also Schiebold et al. 2017).
The evolution of various photosynthetic life styles has been much studied in Epidendroideae-Neottieae (e.g. T. Zhou & Jin 2018; Feng et al. 2016; in particular Lallemand et al. 2019), a tribe where there are all variants from autotrophy to full mycoheterotrophy (the latter has evolved at least three times). There seems to have been rapid evolution at the base of this clade which makes understanding the evolutionary story difficult, but there may not be a simple progression autotrophy → mixotrophy → mycoheterotrophy here (Zhou & Jin 2018; Lallemand et al. 2019). Indeed, Lallemand et al. (2019) found that photosynthesis genes might be under positive selection in mixotrophic species - they suggested that such genes might still be important in fruit development there (see also Suetsugu et al. 2018 in Cymbidium). There are also associations with ECM fungi in mixotrophic/mycoheterotrophic Epidendroideae-Neottieae, autotrophic taxa being associated with saprotrophic and endophytic fungi (Roy et al. 2009; Dearnaley et al. 2012; Lallemand et al. 2019). Members of the Hexalectris spicata complex (Arethuseae) are each associated with different members of the ECM Sebacinales-Sebacinaceae (Kennedy et al. 2011; Weiß et al. 2016), and Barrett et al. (2019b) suggested that there have been four or five independent losses of photosynthesis in this genus alone, interestingly, Hexalectris has an epiphytic ancestry (Sosa et al. 2016). Several species of Russula form both ECM associations with adjacent trees and endomycorrhizal associations with Corallorhiza (Epidendreae-Calypsoineae) (Taylor & Bruns 1999; Freudenstein et al. 2017; see also Z.-H. Li et al. 2020), and in such mycorrhizal networks the tree that is the ultimate source of the orchid's carbon (see also Dearnaley 2007); Corallorhiza includes both leafless species that photosynthesize and those that cannot. Interestingly, in albino individuals of Epipactis helleborine there seems to be some bidirectional flow of carbon between fungus (the ectendomycorrhizal ascomycete Wilcoxina) and plant; green individuals were associated with similar fungi (Suetsugu et al. 2017; see also Kinoshita et al. 2016: Gastrodia-Gastrodieae). However, in Goodyera velutina (Orchidoideae), associated with ECM fungi and cantharellalean rhizoctonia, green individuals were autotrophic and white individuals obtained their C from their cantharellalean, not ECM, associates (Suetsugu et al. 2019). The identity of the fungal associate may change with the establishment of full mycoheterotrophy (Hynson & Bruns 2010). In Cymbidium (Epidendroideae-Cymbidieae) the evolution of mixotrophy and then mycoheterotrophy depends on the establishment of associations between the orchids and ECM fungi (Ogura-Tsujita et al. 2012), and Julou et al. (2005) compared albino and green individuals of Cephalanthera damasonium (Neottieae) and found little difference in fertility between the two, and noted that a number of changes in the albinos were still needed for there to be full mycoheterotrophy.
Yagame et al. (2016) suggested that in Neottia there has been an evolutionary shift from associations with saprophytic/endophytic Sebacinales-Serendipitaceae in the autotrophic taxa to associations with Sebacinaceae in the echlorophyllous mycoheterotrophic taxa. In tropical mycoheterotrophs associations with saprotrophic wood-decay fungi are common (Roy et al. 2009; Garbaye 2013; Hynson 2013; Bayman et al. 2016). Thus non-mycorrhizal but lignin-decaying fungi like the basidiomycete Mycena (Mycenaceae) are members of such associations; Mycena supports the fully mycoheterotrophic Gastrodia confusa (Epidendroideae) in the manner to which it has become accustomed (Ogura-Tsujita et al. 2009 and references), saprotrophic fungi other than "Rhizoctonia" are commonly associated with mycoheterotrophic orchids on Taiwan (Y.-I. Lee et al. 2015: ECM fungi only sometimes involved), and the associates of Galeola [= Erythrorchis] altissima, at up to 10 m or so tall the largest mycoheterotroph known, are largely wood-decaying basidiomycetes (Ogura-Tsujita et al. 2018). The three species of the Australian Rhizanthella (Orchidoideae-Diuridae) are subterranean mycoheterotrophs, the flowers even opening underground (Delannoy et al. 2011); the orchids form an association with the ECM fungi of Melaleuca uncinata (Rasmussen et al. 2015 and references). Here, as is quite frequent in other mycoheterotrophs, the fruits are fleshy and the seeds are crustose (Cameron & van den Berg 2017), in one case at least being dispersed by camel crickets (Rhaphidophoridae: Tachycines elegantissima) like unrelated mycoheterotrophs (Suetsugu 2017, see also 2020).
Finally, Suetsugu and Matsubayashi (2020) recently discovered that there is partial mycoheterotrophy in Apostasia, in Apostasioideae and so sister to all other orchids. They detailed where the fungus primarly involved, Ceratobasidium, was a member of part or full mycoheterotrophic associations in other Orchidaceae, and also was a member of ECM associations, and made the suggestion that partial mycoheterotrophy may be the ancestral condition for Orchidaceae as a whole (Suetsugu & Matsubayashi 2020). See below below for the evolution of the chloroplast genome in mycoheterotrophic Orchidaceae.
The nitrogen metabolism of mycoheterotrophic and partly mycoheterotrophic orchids is poorly understood. However, both groups of orchids are noted for the very high N concentrations in their tissues, and C and N uptake may be linked if nitrogen-rich amino acids move from the fungus to the orchid (Hynson et al. 2013, 2016 for literature; Zimmer et al. 2007; Kuga et al. 2014; Focha et al. 2016).
Any connection between the specificity of the mycorrhizal association and the diversification of Orchidaceae in general (Otero & Flanagan 2006) or speciation in mycoheterotrophic taxa in particular (Kinoshita et al. 2016) is unclear. Some specificity of fungal associations has been noted, thus Shefferson et al. (2005) found quite high specificity between orchids (Cypripedium) and fungal associates (Tulasnella), although less in C. californicum (see also Rasmussen 2002). It has been suggested that differentiation of fungal communities on different species of orchids may contribute to niche partitioning (Waterman et al. 2011; McCormick & Jacquemyn 2013; Jacquemyn et al. 2013 and references). Thus Nurfadilah et al. (2013) found that fungi varied in their ability to utilize nutrients in phosphorus-poor West Australian soils, suggesting that this might help explain diiferences in how common species of orchids were locally. However, Davis et al. (2015) thought that specificity of fungus:orchid relationships was unlikely to explain the endemism of southern Australian orchids, rather, pollination by sexual deception and specific edaphic requirements might be a better explanation. But if the estimate by van der Heijden et al. (2015a) that around 25,000 species of fungi are associated with orchids is confirmed, this may open up all sorts of evolutionary possibilities if at the same time futher questioning ideas of specificity... (for more on the specificity of mycorrhizal associations, etc, see also Bacterial/Fungal Associations below).
The Epiphytic Habitat.
Core Epidendroideae are commonly epiphytic-CAM plants and are highly speciose, including around 19,560 species (figures from Pridgeon et al. 2005, 2009, 2014), i.e., about two thirds of the whole family; Neottieae and some other basal Epidendroideae are not epiphytes (e.g. Freudenstein & Chase 2015). Epiphytic orchids are perhaps the largest group of epiphytes (e.g. Kress 1989; Holtum et al. 2007); they make up ca 70% of all epiphytic flowering plants (Benzing 1983; Zotz 2013), and in the hyperdiverse northern Andes they may comprise 30-50% of the epiphytic species (references in Pérez-Escobar et al. 2017a). Note, however, that Chomicki et al. (2014c) estimated that the epiphytic habit had been acquired four to seven times and subsequently been lost rather more often, although details of the evolution of this trait were unclear. There have been some reversals from epiphytism to the terrestrial habit including in Bletia and its relatives (Epidendreae), one of which, Hexalectris, is mycoheterotrophic and grows in quite dry conditions in North America (Sosa et al. 2016), and there has also been a reversal to the terrestrial habit in Malaxideae (Cameron 2005) and Catasetinae (Martins et al. 2017/2018). Some evidence suggests that epiphytic orchids tend to have narrower ranges than their terrestrial relatives (Martins et al. 2017/2018), although the reverse is true in some other groups (Reimuth & Zotz 2020). For the epiphytic habit and success of the family, see below, and for other major epiphytic groups, see Bromeliaceae, Gesneriaceae, Melastomataceae, Ericaceae and Piperaceae.
Rather little seems to be known about the ecology of epiphytic orchids, for instance, problems that they may face as their host tree grows larger, so changing the conditions of their existence, or more generally, interactions, if any, between host/phorophyte and orchid (Rasmussen & Rasmussen 2018: literature on apparently quite specific associations between orchid and host). Nyffeler and Eggli (2010b) estimated that some 50+ genera and 2,200 species of orchids, or perhaps double that number, especially epiphytic species, were succulent (see also S. Zhang et al. 2018 and Eggli 2020a for general accounts). They have often fleshy leaves that may be terete (Balachandar et al. 2019 - Luisia) or bifacial, and quite often a fleshy stem, whether corm or pseudobulb (Bulbophyllum), although this feature is quite often absent (Freudenstein & Chase (2015). Epiphytic orchids, like other epiphytic plants, have to deal with periodic drought and lack of nutrients (Gravendeel et al. 2004, see also Motomura et al. 2008), as in the dry terrestrial habitats where succulence is also common (see also Figueroa et al. 2008); terrestrial orchids have thinner leaves. Epiphytic orchids often have very thick roots with very well developed velamen and exodermis with tilosomes on top of the living passage cells, pneumathodes are sometimes present, and any root hairs are primarily for anchoring the plant to the twig (e.g. von Guttenberg 1968; Pridgeon 1987: comprehensive; Siegel 2015: a readable account). There may be chloroplasts in the cortical cells (e.g. Benzing 1996). Zotz and Winkler (2013) found that in a number of epiphytic epidendroid orchids both water and nutrient uptake into the velamen was very quick; the velamen dried out slowly, and nutrients moved into the root cortex via the mitochondrion-rich passage cells of the exodermis. However, there was a fair bit of variation in nutrient uptake between the species examined, and overall the function/behaviour of the velamen is not all that well understood.
Associated with the drier conditions of the epiphytic habitat and the succulent habit is the evolution of crassulacean acid metabolism, CAM photosynthesis. A very approximate estimate is that ca 9,700 species of Epidendroideae have CAM photosynthesis (see Winter & Smith 1996b; also Eggli 1991a), and variants of CAM photosynthesis such as CAM-cycling are also common (see Silvera et al. 2008 for Oncidiinae; Winter et al. 2015). However, the actual number of taxa involved is unclear. In a survey of 1,002 Costa Rican orchids, only some 10% of Vanilloideae and Epidendroideae were found to show signs of strong CAM, perhaps 30% more had weak CAM; CAM was not found in Orchidoideae and Cypripedioideae (Silvera et al. 2010a). Similarly, in a survey of 1079 orchids - mostly Epidendroideae, mostly Colombian, and three quarters epiphytic - only 8.9% (9.4% of the epiphytic species) had the carbon isotope signature of CAM plants (Torres-Morales et al. 2020). Such figures suggest that overall there are somewhat fewer than 2,500 CAM orchids. Givnish et al. (2015) thought that CAM might have evolved four times or so in the family, Martin et al. (2010) suggested that CAM has evolved perhaps ten times in Orchidaceae, but also with reversals to C3 photosynthesis, and there were also intermediates, while M.-H. Li et al. (2019: support along the spine tends to be weak) proposed some eight origins in Dendrobium alone. In this last study, the first origin of CAM was dated to (28.9-)21.9(-16.0) Ma in the Asian clade, and in general origins there were older than in the Australasian clade (Li et al. 2019). Silvera et al. (2009) found CAM radiations in Cymbidieae-Oncidiinae and Epoidendreae-Laeliinae in particular.
Cauline pseudobulbs, common in epiphytic orchids, may carry out CAM even although they lack stomata. CAM occurs in Bulbophyllum minutissimum, however, since the pseudobulb of Bulbophyllum is a modified leaf, even if lacks a blade, one presumes there are stomata (Kerbauy et al. 2012 and references). The photosynthetic pathway in root and pseudobulb and in the leaf may be different, the former being C3 while the latter is CAM (Martin et al. 2010), or vice versa (Rodrigues et al. 2013). Adoption of CAM is predominantly by epiphytic Epidendroideae growing at low altitudes and drier conditions (Silvera et al. 2009; Kerbauy et al. 2012; M.-H. Li et al. 2019: cooling perhaps also involved) and has been linked to the Caenozoic radiation of that subfamily (Silvera et al. 2009). However, CAM photosynthesis has evolved perhaps four times (and reversed once) in terrestrial Eulophiinae (Epidendroideae) (Bone et al. 2015b). In the Madagascan Eulophiinae adoption of CAM may have allowed the orchids to move into drier habitats (Bone et al. 2015b). Species of Madagascan Angraecum (Vandeae) growing in humid conditions/more substrate have δ13C values suggesting that C3 photosynthesis is going on in the plants, while in those growing in drier conditions/less substrate the values suggest C4 photosynthesis (Kluge et al. 1998). Gene duplication has been implicated in the functional diversification of genes like phosphoenolcarboxylase that are involved in CAM photosynthesis (Silvera et al. 2014), although Deng et al. (2015) suggested that the number of duplicate genes may be irrelevant as regards photosynthesis type. See also Bräutigam et al. (2017) and Hermida-Carrero et al. (2020: molecular evolution of RuBisCO) for the evolution of CAM photosynthesis and Males and Griffiths (2017) for the stomatal biology of CAM plants.
Another general problem faced by epiphytic plants is damage to tissues caused by UV-B radiation. Twig epiphytes in particular, concentrated in a clade of the New World Epidendroideae-Cymbidieae-Oncidiinae, face such problems. They grow on twigs less than 2.5 cm in diameter and in very exposed and high light conditions. Recent work suggests that chalcone synthase genes can be induced by UV-B light in the root tips of epiphytic orchids, and as a result UV-B-absorbing flavanoids are synthesised (Chomicki et al. 2014c: for sunlight and epiphytism, see also Bromeliaceae). A leafless orchid was included in this study and it showed behaviour similar to that of the two leafy epiphytic taxa examined.
Other than succulence and associated CAM photosynthesis and the ability of a few epiphytic orchids to capture humus, whether in baskets formed by negatively geotropic roots (e.g. Grammatophyllum) or by leaves (Zona & Christenhusz 2015), orchids would seem to have few obvious adaptations to growing in an environment where water is often at a premium. A recent study examining phorophyte (host tree) preferences of orchids in southeast Mexico found that orchids did not prefer trees with fissured bark, where water would seem to be able to remain in the fissures. Rather, the amount of water persisting after the excess drained away was linked to the density of porose structures in the bark, and these trees were preferred (Zarate-García et al. 2020).
Mycorrhizal associations are usually less common in epiphytes than in other plants (e.g. Janos 1993; Desirò et al. 2013). However, the basidiomycete Sebacinales-Serendipitaceae and Tulasnellales (= Cantharellales) are ECM associates of neotropical epiphytic orchids. Species of Tulasnellaceae, at least, colonize more than one species of orchid (Kottke et al. 2008; see also Martos et al. 2012; Gowland et al. 2013; Balachandar et al. 2019), while in montane South America mycorrhizal Serendipitaceae are in clades close to but separate from clades that form distinctive modified ericoid mycorrhizae in Ericaceae growing in the same habitats (Setaro et al. 2013). Perhaps surprisingly, it was found that on Réunion relationships between epiphytic fungi (including Ceratobasidiaceae) and their host epiphytic orchids (34 spp., angraecoids, most Angraecum itself) were nested, but not those in terrestrial orchids (25 genera); there were different fungi in different habitats, and low specificity in the terrestrrial orchid-fungal associations (Martos et al. 2012). Basidiomycete fungi are to be found in the photosynthetic roots of the leafless epiphyte Dendrophylax lindenii (Chomicki et al. 2014b). In addition to the implications such mycorrhizal associations have for the nutrition of the epiphytic orchid, there may also be associations between aerial roots of the orchids and nitrogen-fixing cyanobacteria and interactions with other bacteria from the rhizosphere (Teixeira da Silva et al. 2015: focus on Dendrobium).
The twig epiphytes common in Oncidiinae are particularly distinctive. Their seed coats have little grapnel-like structures, perhaps aiding in their attachment to the twigs (Chase & Pippen 1988). The plants are very small and may mature within a year (Chase 1987; Chase and Palmer 1997; Neubig et al. 2012a); indeed, many of these epiphytes are exposed to light immediately on germination, rather than having an initial slow-growing subterranean mycotrophic phase (Leake & Cameron 2012). Chase et al. (2005) found that genome sizes in these annuals was not particularly small when compared with those of their immediate relatives. Their leaves are isobifacial or otherwise strongly laterally flattened and are arranged like a small fan or in two ranks (the psygmoid habit) and the plants have no pseudobulbs. All in all, they look like very young plants of other Oncidiinae and are more or less paedomorphic (Chase 1987; Neubig et al. 2012a for references: see Bromeliaceae-Tillandsioideae for a comparable situation).
The leaves of some epiphytic Epidendroideae-Vandeae in particular are very small and not photosynthetic and/or are soon deciduous, and the vegetative plant consists largely of photosynthetic roots. These roots may be quite thick (ca 5 mm across) and terete, as in Dendrophylax, while those of the aptly named Taeniophyllum are distinctively flattened (e.g. Carlsward et al. 2006b). There are over 200 species of leafless Epidendroideae, all epiphytes, and overall leaf loss is estimated to have occured 20 or more times in Orchidaceae (Freudenstein 2012). Cortical cells of the roots of these epiphytes have chloroplasts, but how carbon dioxide and water flux are controlled here is unclear especially since the roots lack stomata, however, the aeration units there may be stomata analogues (Benzing et al. 1983; Cockburn et al. 1985; Benzing 1996). CAM occurs in the stomata-less roots of leafless orchids like Campylocentrum tyrridion (Kerbauy et al. 2012; Winter et al. 2015). In general, photosynthesis in orchid roots, including those of many leafy epiphytic taxa which also have green roots, is poorly understood.
Epiphytic orchids in general have smaller genomes that those of their terrestrial relatives (Chase et al. 2005), although the significance of this is obscure (epiphytic ferns tend to have quite large genomes...). However, if nitrogen is at a premium (see also carnivorous plants) reduction in genome size - and hence in the amount of nitrogen used in its synthesis - to a functional minimum might be an advantage (Vesely et al. 2013).
Interestingly, there are spiral-crack root hairs, root hairs whose walls break down and form a ribbon-like spiral, in some epiphytic Orchidaceae (e.g. Stern 2014; Bernal et al. 2015). In Araceae such hairs are thought to help dissipate energy from strains on the roots that are likely in climbers (X. Yang & Deng 2016) - and such strains are also likely in epiphytes, too, although in Orchidoideae-Spiranthinae, at least, not all the species with such hairs are epiphytes (Bernal et al. 2015); see also Posidoniaceae.
Other issues: Myrmecophytism is known from Myrmecophila (Epidendroideae), which grows in dry and open environments, even on sand dunes (Rico-Gray et al. 1989; Pridgeon et al. 2005).
Flowering may be stimulated by fire in a number of ground-dwelling Orchidoideae, the trait perhaps originating as long ago as 60 Ma (Lamont & He 2017; Lamont et al. 2018a).
Pollination Biology & Seed Dispersal.
The literature on orchid flowers and their pollinators is very extensive - an understatement - and only some is mentioned below. For summaries of pollination in Orchidaceae, see van der Cingel (1995, 2001), Endress (1994b), Biol. J. Linnean Soc. 173: 713-773. 2013, Pridgeon et al. (1999, 2001b, 2003, 2005, 2009, 2014), Valencia-Nieto et al. (2018: Epidendreae), etc. - and of course the classic study by Darwin (1862a) is still worth reading (see also Yam et al. 2009; Edens-Meier & Bernhardt 2014b). For a general discussion on floral evolution in the family, with an emphasis on terata and homeosis s.l., see Rudall and Bateman (2002); Rudall and Bateman (2004: outgroup a Hypoxis-type flower, but this is of no consequence) emphasize the various processes involved.
Orchid flowers may be notably long-lived (even months), although some last only for a single day; flowers that are pollinated by deceit (see below - perhaps very common here) tend to live longer than flowers that offer a reward (Nunes et al. 2017 and literature). Flowers are commonly resupinate, the ovary being twisted about 180°, the labellum ending up in the abaxial position (Ernst & Arditti 1994; Yam et al. 2009 for reviews). However, the degree of resupination often varies within a plant when the inflorescence is arching, all flowers of the one inflorescence ending up being oriented so that their labellum is in the same position with respect to gravity, with the ovary sometimes being twisted 360° (as in Angraecum, etc.) or not at all. Indeed, the labellum may have switched from abaxial to adaxial in position ca 5 times in Angraecum alone, speciation rates being higher in clades with the latter position (Andriananjamanantsoa et al. (2016). Fischer et al. (2007) discuss the variety of ways - of which twisting of the pedicel is but one of the mechanisms involved - that flowers in the speciose Bulbophyllum present themselves in the Malagasy region. Catasetum has resupinate staminate flowers, but the carpelate flowers are not resupinate (see also below). Flowers of Stelis, which commonly have a very short inner perianth that may appear to be little differentiated, may be presented with the odd member of the outer perianth whorl abaxial (Karremans 2019). In genera like Calopogon the flowers are never resupinate, and all flowers on the erect inflorescence show "normal" monocot orientation, the labellum being adaxial. Koopowitz (2017) discussed the absence of resupination s. str. (= twisted ovary) in basal clades like Cypripedioideae, etc., but the flowers are still presented to the pollinator inverted, i.e. with the median sepal adaxial and the median petal, the laballum, abaxial.
The outer and inner whorls of the tepals are more or less distinguishable, and the most conspicuous element of the flower is often the labellum, a member of the inner whorl of tepals, which shows a truly remarkable diversity of form and colour (Rudall & Bateman 2002; see also 2004); duplication of B-class genes may be involved (Mondragón-Palomino & Theißen 2008; Mondragón-Palomino 2013 and references). The column is formed from the androecium and stigma/style, and there is generally only a single stamen with the pollen grains variously aggregated into pollinia. The spatial relationships of the labellum and column in particular force the pollinator to approach the flower in a particular way, and in general, pollinaria are usually very precisely placed on the pollinator, closely related orchid species differing in exactly where their pollinaria are placed (e.g. Maad & Nilsson 2004). After the pollinarium is attached to the pollinator, the pollinia may move, so bringing them into the proper position for pollination; for pollinia, pollinaria, and pollen deposition - not always in one go even when there are pollinia, e.g. Listera (= Neottia, Epidendroideae), see Rasmussen (1982), Freudenstein and Rasmussen (1996, 1997), Nazarov and Gerlach (1997), Johnson and Edwards (2000), Pacini and Hesse (2002), Freudenstein et al. (2002), Harder and Johnson (2008), Selbyana 29: 1-86. 2008, and so on. The plesiomorphic condition for Orchidaceae is to have elastoviscin (quite different from the viscin threads of, say, Onagraceae) associated with the pollen grains. It is very similar to pollenkitt, although tapetal plastids seem not to be involved in its synthesis, and makes up the stipe of the pollinaria in some orchids, or it can be entirely lost (Still & Wolter 1986).
A final distinctive feature of many orchid flowers is that the ovules are usually not fully developed - and may not even be recognizable - at anthesis, and fertilization is then delayed relative to pollination, as in Cypripedium. The time between pollination and fertilization ranges from four days to ten months (in Vanda) in the family, the normal time being one week to six months (Wirth & Withner 1959, Yeung & Law 1997; also Sogo & Tobe 2005, 2006d for references; Duarte et al. 2019: ?Apostasioideae). Even after fertilization, it may be a month before embryo development begins, as in Sarcanthinae (Wirth & Withner 1959 for references). In some species there may be ovules with developing embryo sacs in capsules that also have more or less mature seeds (Duarte et al. 2019).
Self pollination in orchids may be quite common (Gamisch et al. 2014 for a review). The bee-mimic Ophrys apifera may self-pollinate if not visited by bees; there the pollinia curve downwards and meet the stigma. There are other selfing mechanisms, too, as in Paphiopedium parishii where the contents of the anther liquefy and slop on to the stigma (L.-J. Chen et al. 2013). In Madagascan Bulbophyllum selfing varies infraspecifically and is associated with the loss of the rostellum, as it often is elsewhere in the family (Gamisch et al. 2014; see also e.g. Peter & Johnson 2009). For selfing in Angraecum from the Mascarenes, an area where there are no sphingid pollinators, see Michenau et al. (2014: many other orchids there also self, see references).
In the following brief discussion on orchid pollination, I emphasize first rewards, then the pollinator, with some other issues mentioned at the end. For pollination, see also van der Pijl and Dodson (1966) and Claessens and Kleynen (2016: European orchids), and for pollination in Vanilloideae, see Pansarin (2016).
Rewards - or Lack Thereof.
The plesiomorphic condition for the family may be to lack nectar (Jersáková et al. 2006). It has been suggested that about one third or so of orchid species - estimates range from 6,500 to 10,000 or even more - have some kind of deceit 0r mimicry-type pollinations systems (Safni 1984; Ackerman 1986; Schiestl 2005, 2010 for reviews, the latter brief; Renner 2006a: rewardless flowers in general; Schlüter & Schiestl 2008: molecular mechanisms; Peakall 2009: deceit and speciation; Chase 2009: deceit in Oncidiinae; Schaefer & Ruxton 2010: plant exploitation of the pollinator's perceptual biases; Gaskett 2011: the pollinator's point of view in sexual deception; Xu et al. 2012; Pinheiro & Cozzolino 2013: deceit in Epidendrum). Apostasioideae provide pollen as a reward for pollinators (Kocyan & Endress 2001), but deception may well have occurred in the common ancestor of the rest of the family (Weston et al. 2014; Givnish et al. 2015). However, species with rewards may be more common than is thought (Karremans et al. 2015; Pansarin et al. 2021), while Shrestha et al. (2020) emphasise that in fact we have very little idea as to the proportion of orchids that practice deceit pollination.
Deceit comes in various guises, from sexual deceit, where the orchid mimics a female insect and pollen exchange occurs during pseudocopulation (e.g. Ophrys below), to domicile deceit, as in species of Serapias (Orchideae: Bellusci et al. 2008 for a phylogeny) and Cypripedium (Cypripedioideae: Pemberton 2013) that attract pollinators by mimicking a nest hole. More generally, flowers pollinated by deceit appear to have rewards, whether a fungal body or carrion where insects can lay eggs, but in fact lack them (Kagawa & Takimoto 2015 and references). Sonkoly et al. (2016) found that orchids with deceit pollination may set fewer fruits than orchids with other sorts of pollination mechanisms, but they set more seeds per fruit, so similar numbers of seeds per plant are produced. See also the section on pollinators below, especially dipterans.
There are more complex situations where flies (Drosophila in this case) are attracted to flowers by aggregation pheromones, but there is nectar reward and the flies may copulate when on the flower (Karremans et al. 2015), or the flower of Gastrodia pubilabiata looks like the fruiting body of the ECM fungus (Mycena) that is associated with it, and which may even be growing nearby (Suetsugu 2018). Apparently rewardless flowers may well turn out to have rewards on closer examination, for instance, some Maxillariinae like Camaridium cucullatum did in fact produce lipids or resins on their labella (Davies & Stpiczynska 2019; Shrestha et al. 2020), while 75% of the small-flowered Oncidiinae examined by Pansarin et al. (2021) produced oil, nectar or perfume, the latter for euglossine bees.
Flowers of the European Ophrys (Orchidoideae-Orchideae) are well known for deceit pollination, their labellum mimicking female bees and wasps (e.g. Kullenberg 1961; Paulus 2006). They also produce chemicals that are very similar to insect pheromones; alkenes (hydrocarbons with at least one double bond) are part of the chemical component of this mimicry (e.g. Stökl et al. 2009; Ayasse et al. 2011; S. Xu et al. 2012; Joffard et al. 2020). Morphology and scent together enable the Ophrys flower to mimic female insects (Cortis et al. 2009 and references), pollination occurring as male bees and wasps in particular attempt to copulate with the flowers (Kullenberg 1961; Kullenberg et al. 1984 and references). Barriers to crossing - floral form and scent again - are pre-zygotic, acting before pollination, indeed, few deleterious effects of hybridization, which occurs in the wild, have been noted (S. Xu et al. 2011). Scent chemicals are common in related genera as well (Schiestl & Cozzolino 2008), and Ophrys is part of a larger clade in which food deception seems to be the basic condition (Inda et al. 2012). However, there is currently much discussion about species limits in Ophrys, with estimates of species numbers ranging from 16 to 252 (Bateman et al. 2006a, esp. 2011a, 2018a; Devey et al. 2008; Vereecken et al. 2011; Bradshaw et al. 2010 and Vignolini et al. 2012a: labellum colour due both to cell structure and pigment; Delforge 2006 and Alibertis 2015 [half the book!]: photographs of the species/"species"). Paulus (2006: p. 315) thought that "species formation in Ophrys always proceeds with the aquisition of a new species of pollinating males", and species that had different pollinators might show "genic rather than genome-wide differences", speciation had barely begun (Sedeek et al. 2014: p. 6202). If this approach guides the delimitation of species, then emphasis on monophyly - there are only a few more or less strictly monophyletic species (Bateman et al. 2018a) - will be side-stepped. Joffard et al. (2016) discuss floral scent bouquets in these orchids and species limits. Rapid diversification in the Pleistocene accompanied shifts to different pollinators, from wasps to apid or andrenid bees (Breitkopf et al. 2015).
Around 100 species of Australian Caladenia (Orchidoideae-Diuridae) are pollinated by male thynnine wasps (Phillips et al. 2009, other articles in Australian J. Bot. 57(4). 2009; see also Brown & Brockman 2015). In another Australian genus, Chiloglottis (also Diuridae), where scent also plays a role in maintaining reproductive isolation (Peakall & Whitehead 2013), there is a fair degree of congruence between the phylogenies of the orchids and the deceived wasps (Mant et al. 2002, 2005; see also Weston et al. 2011; Miller & Clements 2014). In both cases understanding species limits is critical; there seem to be a number of cryptic species, hybridization occurs, etc. (see also Jones et al. 2001; Griffiths et al. 2011). In such sexually-deceptive orchids both morphological and genetic differences between species or even genera are slight (Schiesl 2005 and references; Mant et al. 2005; see also below) and post-pollination reproductive barriers may be nonexistent (Whitehead & Peakall 2014).
Chemical signalling between plants and insects involved in pollination occurs in many situations, not only enhancing floral mimicry in pseudocopulation. Thus wasps may be attracted to orchid flowers that produce chemicals similar to those produced by damaged plant tissue - the wasps visit the flower expecting to find caterpillars, but pollination occurs instead. Similarly, Dendrobium sinense, pollinated by a hornet, has a floral bouquet that includes the same chemicals as in the alarm pheromones of Apis, which the hornet commonly catches (Brodmann et al. 2009). The volatile emissions that some orchids produce suggest carrion, so attracting insects looking to lay eggs in the non-existent carrion but that pollinate the flowers in their search (see Jürgens et al. 2013 for the syndrome).
Other kinds of food deceit are quite common, as with pollen mimicry in Vanilloideae-Pogonieae where it characterises a clade that includes temperate species; pollen is apparently available for removal (Pansarin et al. 2012). Nectar deceit is also common in Caladenia (Phillips et al. 2009). A number of species of Epidendroideae-Oncidiinae have flowers like those of oil-producing Malpighiaceae, q.v.; they have radiating, clawed, yellow or purple "petals" that are similar in both shape and in colour, bee-UV-green, to petals in flowers of Malpighiaceae. Overall, there may be a Batesian mimicry system here, both groups of plants being visited by bees like Centris, although the orchids often have no reward for the bee (Neubig et al. 2012a; esp. Papadopulos et al. 2013; c.f. in part Pansarin et al. 2021; see also below). The mimicry unit of the orchid is formed largely by the labellum, the column being equivalent to the banner petal of a malpighiaceous flower. M. P. Powell (in Neubig et al. 2012a) has estimated that such mimicry may have evolved at least 14 times within Oncidiinae, indeed, it may be both lost and regained (Papadopulos et al. 2013). Other Oncidiinae mimic Calceolaria, another oil flower (Neubig et al. 2012a). Floral mimicry is also known from the largely Australian Thelymitra which has sub-polysymmetric flowers (Edens-Meier & Bernhardt 2014a). Orchid flowers that are attractive, but that lack any rewards, may have polymorphic flowers, if the pollinator is not that good at discriminating colours (and is a rather slow learner), or more continuous variation, if the pollinator is better at distinguishing colours (Kagawa & Takimoto 2015).
Flowers of many orchids do have rewards for the pollinator, and such flowers have frequently been derived from flowers lacking rewards (Cozzolino et al. 2001; Cozzolino & Widmer 2005; Smithson 2009; Pansarin et al. 2012; S. D. Johnson et al. 2013). Thus in the speciose African Disa (Orchidoideae), there have been several transitions from deceit to nectar rewards, and loss of nectar, and independent gains and losses of spurs, but all without having much of an effect on diversification rates (S. D. Johnson et al. 2003) or on mating (selfing vs wide outcrossing), etc. (Hobshawn et al. 2017; see also Smithson 2006). The production of rewards may also be derived in Vanilloideae-Pogonieae (c.f. Pansarin et al. 2012), mimics of Malpighiaceae in Oncidiinae (see below), etc..
Pollen alone is collected from flowers of Apostasioideae (there is buzz pollination in Apostasia), and from some Vanilloideae (Pansarin et al. 2012). Nectar flowers are quite common (Bernadello et al. 2007 and references), and although Orchidaceae do not have septal nectaries, nectar spurs are scattered in the family. For spurs, nectariferous and otherwise, in Orchidoideae-Orchidinae, including Habenaria, see Bell et al. (2009); the flowers of African Satyrium are not resupinate and have twin nectar spurs (S. D. Johnson et al. 2011a). For other nectar spurs, which develop from the adaxial sepal, in the largely Australian Diurideae, see the summary in Weston et al. (2011, 2014), and here various kinds of mimicry, and nectar production, sometimes from the labellum, have evolved, and then perhaps been lost many times. Spurs are common in Vandeae, as in Angraecum (Angraecinae, see above), and Aeridinae (Topik et al. 2005), for example. Tissue on the tepals may also produce nectar (Davies et al. 2005). Hobbhahn et al. (2013) discuss the evolution of nectaries of various types (a secretory nectariferous epidermis is here descibed as being "recapitulatory") in Disa, which has happened some eight times here alone.
Resins and oils are also quite common rewards; for a summary of oil flowers in Orchidaceae, which have evolved probably at least a dozen times, eight times in Maxillariinae alone, see Renner and Schaefer (2010, also references in Arévalo et al. 2017b); flowers of some species mimic the presence of resin rewards (Whitten et al. 2007; Davies & Stpiczynska 2012, 2017). In a number of other species of Maxillaria hairs on the labellum contain protein and perhaps also starch and function as pseudopollen, so rewarding the pollinator (Davies et al. 2000; Davies 2009; also Arévalo et al. 2017b for labellar micromorphology in Mormolyca-Maxillariinae). Maxillariella produces small quantities of resins along with sugars and/or proteins, etc., that may serve as a food reward, interestingly, the main components of resins in other Maxillariinae were not found here. The flowers of orchids that have oil as a reward may show convergence with those of other oil-pollinated plants. Thus some 70 or more species of Oncidiinae have elaiophores, often on the labellum; these may be epithelial or tufts of unicellular secretory hairs (Blanco et al. 2013; Davies et al. 2014; Tölke et al. 2019 and references) and be visually similar to elaiophores on the calyx of Malpighiaceae, or the flower as a whole may be like those of Malpighiaceae. The distinctive oil secreted is also very similar to that produced in the flowers of Malpighiaceae (see above; Reis et al. 2007 and references), and there may be some kind of Müllerian mimicry system here (Papadopulos et al. 2013), but such systems are difficult to categorise (see also Policha et al. 2014); Centris and Tetrapedia visit oncidiine flowers with different floral syndromes (Gomiz et al. 2017). Pollination of some South African Orchidoideae-Coryciinae (e.g. Disperis) is by oil-collecting bees; the flowers have paired, pouch- or spur-like structures like those of another local oil plant, Diascia (Scrophulariaceae: Pauw 2006). The South African Huttonaea, perhaps immediately unrelated, also has oil flowers (Steiner 2010); Steiner et al. (2011) analyzed scent composition of many southern African oil-secreting Diseae. All told, oil flowers have been reported from 8 subtribes, of which Epidendroideae-Cymbidieae-Oncidiinae have by far the most examples (Possobom & Machado 2017 and references); see also Chase et al. (2009) and Steiner (2010) for oil flowers.
Male euglossine bees are pollinators of many species of neotropical orchids (see below) which they visit to collect fragrances that they subsequently use in their courtship displays.
Fly pollination is common (Christensen 1994; Siegel 2016 for a readable summary), especially in Epidendroideae. Thus the very speciose and largely Old World Bulbophyllum (Epidendreae-Bulbophyllinae) often has dark, purplish-coloured flowers, the labellum is mobile, and there may be dangling structures (hairs of various kinds, labellum tips), and it attracts a variety of flies (Vogel 2001: also Pleurothallidinae; see also A.-Q. Hu et al. 2019). A number of taxa have sweet, fruity scents and lighter-coloured flowers and are pollinated by fruit flies - which may also be commercially important pests (Tan 2008 and references, see also Texeira et al. 2004; Fischer et al. 2007 for resupination there). Stpiczynska et al. (2015, 2018 and references) found some African species to have scented flowers and nectar (secreted by the labellum), or lipids as a reward, and the labellar tissue might be aerenchymatous, presumably increasing its mobility. Some species have flowers with a carrion scent suggesting pollination by necrophagous insects, as Siegel (2016: p. 87) noted of the flowers of B. fletcherianum, they smell "like a herd of dead elephants". However, as with other megagenera, little is really known about pollinators and floral rewards, yet the floral diversity of the genus beggars description (see e.g. the illustrations in Vermuelen et al. 2015). A rather similar set of features, including a variety of scents, a mobile labellum, etc., characterize the new World Pleurothallidinae, and again fly pollination, especially by drosophilids, is prevalent, perhaps contributing to diversification, Karremans & Díaz-Morales 2019). In the large New World genus Lepanthes, pollination during pseudocopulation with fungus gnats (dipterans, often Sciaridae) has been reported (Blanco & Barboza 2005). How this system might function is unclear since there is no obvious connection between the morphology of the orchid flower and that of the fungus gnat (Singer 2011). Biting midges have been implicated in the pollination of the related Trichosalpinx, again, the flowers have a syndrome very like that mentioned above for Bulbophyllum (Bogarín et al. 2018). Fungus-visiting drosophilids pollinate Dracula, which can have a distinctively-patterned outer perianth as well as a labellum that looks (and smells) very much like a fungus with gills, and other flies are also involved (Policha 2014; Policha et al. 2014, esp. 2016). Stimulation of the labellum by ?flies visiting the flowers of Porroglossum causes it to snap shut, imprisoning the insect against the column whence they remove the pollinaria, and the trap reopens after some minutes (Pridgeon et al. 2005; McDaniel & Cameron 2016). Indeed, a variety of dipteran groups pollinate orchids, sometimes nectar is a reward, or the orchid simulates decaying material or a fungus (sapro- or mycomyophily), or insects, etc., captured by another predator, but that serve as food for kleptoparasitic flies (kleptomyophily). Such modes of pollination are likely to predominate in the some 4,000+ species of Epidendroideae-Pleurothallidinae, to which Lepanthes and Dracula belong (Pridgeon et al. 2005 and references; Karremans et al. 2016; Davies & Stpiczynska 2017: Mormolyca s. str., = Maxillaria s.l.; Bogarín et al. 2018). Here self incompatability tends to be developed, as in some other Epidendroideae (Borba et al. 2011; Duque-Buitrago et al. 2014; Karremans et al. 2015). Pollination by Drosophila and Scatophaga is also known in Cypripedium (P. Li et al. 2012; see Edens-Meier et al. 2014 for Cypripedioideae in general), while carrion flies pollinate Satyrium pumilum (Orchidoideae-Diseae: van der Niet et al. 2011). See also above (Rewards - or lack thereof).
Moth, butterfly, and even bird pollination are also well known in the family. Angraecum sesquipedale (Epidendroideae-Vandeae), from Madagascar, is a classic example of moth pollination. There the spur is 30-45 cm long, and the pollinator for long remained unknown, although Darwin (1862) suggested that some moth with a proboscis that long would be found. Indeed, Xanthopus morgani praedicta, with a proboscis about 25 cm long, was subsequently discovered (Nilsson et al. 1987; Nilsson 1988: Wasserthal 1997; Arditti et al. 2012); see Micheneau et al. (2010) for pollination in the over 200 species of angraecoid orchids. For the great floral and pollinator diversification in some genera of Orchidoideae-Orchidinae, including Disa, see S. D. Johnson et al. (1998, 2013) and Bytebier et al. (2007); Hapeman and Inoue provide an extensive discussion of pollination in Platanthera, a genus that has turned out to be polyphyletic (Jin et al. 2014).
It has been estimated that perhaps 60% of Orchidaceae are pollinated by bees (Schoonhoven et al. 2005), whether deceived or not. N. H. Williams (1982) discussed the general importance of male euglossine bees in particular in the pollination of neotropical Epidendroideae (see also Roubik 1988, 2014). There are some 190-230 species of orchid bees and they pollinate perhaps up to 25% of tropical American Orchidaceae, hence their common name, orchid bees. However, estimates of the numbers of orchids pollinated by orchid bees vary considerably. Pollination by euglossine bees is especially common in orchids growing at lower altitudes, and anywhere from 900-2,000 species may be involved (Cameron 2004 and references; Zimmermann et al. 2009; Ramírez et al. 2011 - Photo: bee pollinators). Ramírez (2009) thought that some 700 species of orchids had fragrances that attracted male bees, about 85% of all plants with such fragrances; another estimate is that perhaps 2,000 species of Epidendroideae (i.e. almost all Stanhopeinae, Zygopetalinae and Catasetinae) are visited by male euglossines for fragrances (see e.g. N. H. Williams 1982; numbers from Pridgeon et al. 2009). However, very little is known about the pollination of most of these orchids, and Nunes et al. (2017) found that the Zygopetalum species they examined were pollinated by bumblebees and those of Dichaea by weevils, although both genera had been thought (tentatively) to be pollinated by orchid bees (Pridgeon et al. 2009). For further discussion on euglossine pollination, see Clade Asymmetries.
Orchid bees are vigorous fliers and may range up to 23 km from their nests (Janzen 1971). Male bees pollinate the flower as they collect fragrances that they store in their hind tibial pockets, these fragrances perhaps being involved in pre-mating isolation mechanisms in the bees. Closely related and sympatric species of Euglossa did show greater disparity in the fragrances they preferred than might be expected, but overall, the most dominant compounds in the fragrances were highly homoplasious (Zimmermann et al. 2009). Most of the fragrances that the bees pick up from the orchids can also be found elsewhere. Pollination in Gongora (Cymbidieae) occurs as the bee slides down the column having lost its hold on the epichile, slipping on the wax that covers the epidermis (Adachi et al. 2015; c.f. Nepenthes). Hetherington-Rauth and Ramírez (2015, 2016) found that species in different sections or subgenera might have similar scent bouquets, but this was less likely in more closely-related species, indeed, in some species there were sympatric chemotypes that attracted different species of bees. Coryanthes has remarkable flowers in which the pollinating bees cannot grasp the smooth surfaces, become wetted by secretions from the base of the column, fall in to liquid in the apical part of the labellum, and crawl slowly out between the apex of the labellum and that of the column, pollination occurring then (Gerlach 2017). Finally, focussing on Cirrhaea and Stanhopeinae, Pansarin et al. (2018) found that one species of orchid could be pollinated by two or more species of bees, and one species of bee visited two or more species of orchids. For orchid bees and pollinated orchids, see also Feinsinger (1983), who thought that reciprocal evolution was unlikely.
That Catasetinae, Catasetum in particular, are pollinated by male euglossine bees is well known (Darwin 1862; Chase & Hills 1992; Pérez-Escobar et al. 2015, 2017b for phylogenies; Gerlach 2013), and its flowers are quite remarkable, even for an orchid. Here staminate flowers are resupinate and carpelate flowers are not, and there are many other striking differences, especially in labellum morphology, between the two; indeed, plants with staminate and carpelate were once placed in separate genera, Myanthus and Monachanthus respectively. Bees, mostly Euglossa and Eulkaema, visit the flowers of Catasetum for fragrances, different species of orchids tending to have different combinations of frangrances which cuts down the number of species of bees visiting them (Milet-Pinheiro and Gerlach 2017). Franken et al. (2016) describe the osmophores. However, details of floral scent chemistry and both complex and poorly understood (see also Milet-Pinheiro et al. 2015). The attachment of the pollinaria on the bees is by a trigger-activated explosive mechanism (Nicholson et al. 2008). The bee is startled, and Romero and Nelson (1986) suggested that as a result it subsequently avoided staminate flowers, hence the very different morphologies of the carpelate flowers, which, however, are more similar between the species: "The battered pollinator will remember the negative experience with the staminate flower" (Gerlach 2012: p. 39). A final wrinkle is that the kind of flower produced is determined, at least in part, simply by light, bright light tending to favour the production of carpelate flowers (Gregg 1975); Pérez-Escobar et al. (2015) found that environmental sex determination had evolved three times here, 164 species being involved (Catasetum, Cynoches, some Mormodes).
Although euglossine bees are effective pollinators and the morphologies of the flowers that they pollinate are often nothing short of unbelievable, the relationships between orchids and bees are non-specific, particularly on the side of the bee (Ackerman 1983; Cameron 2004; Ackerman & Roubik 2012), although Stebbins (1970) thought that both bee and orchid speciated extensively because of their association. Importantly, crown-group euglossines can be dated to 42-27 Ma, with especially rapid diversification 20-15 Ma (Ramírez et al. 2010) or (35-)28(-21) Ma (Cardinal & Danforth 2011). (Stem-group euglossines are Cretaceous in age - e.g. Grimaldi & Engler 2005.) The orchids these bees pollinate speciated about 12 Ma later, (31-)27-18(-14) Mya (Ramírez et al. 2011) or 22-16 Ma (Givnish et al. 2015: two origins), the estimates being from Catasetinae and Zygopetalinae plus Stanhopeinae, immediately unrelated clades. Pollination by euglossine orchid bees may be largely restricted to two clades in core Epidendroidea. Lubinsky et al. (2006), noting that a number of genera in the three basal clades of orchids had aromatic fruits, and that orchid bees pollinated Vanilla, even thought that orchid-orchid bee relationships could have involved both pollination and seed dispersal, the latter even being the ancestral condition for the family (see also Rodolphe et al. 2011).
The connection between orchid-pollinator relationship and orchid diversification remains a matter of active discussion. Tremblay et al. (2005) reviewed the evolutionary consequences of the diversity of the pollination mechanisms of Orchidaceae and the remarkable variation shown by their flowers. Orchid diversification is often explained in terms of the close association between pollinators and individual species of orchids, whether or not cospecation or coevolution is involved, and pollination relationships are usually thought of as being very precise. Reproduction in orchids may often be pollinator-limited (Tremblay et al. 2005), with few flowers on an inflorescence producing seeds, however, the production of huge numbers of seeds by each fruit may compensate for this - as Pérez-Hérnandez et al. (2011) noted, orchids "specialize in chance". Interestingly, nectarless orchids have a lower reproductive success that orchids that have nectar as a reward (Kindlemann et al. 2007: sample size small, latitude unimportant), and reproductive success of tropical orchids may be lower than that of their temperate relatives, perhaps because it is more difficult for the pollinator to find the orchid in diverse tropical vegetation (Kindlemann et al. 2006); these patterns will interact with factors like pollinator specificity, etc..
The presence of well-developed and effective premating/prezygotic barriers in many Orchidaceae may have obviated any pressure for the selection of postmating barriers (e.g. Whitehead & Peakall 2014). As a result, artificial crosses are often easy to make (some 110,000 have been made), and hybrids may have three or more genera in their parentage, although how these will look when generic boundaries are redrawn is unclear. Hybridization in the wild - and sometimes also polyploidy - has been noted in a number of cases, e.g. Epidendrum (Marques et al. 2014), Ophrys (Xu et al. 2011) and Chiloglottis (Miller & Clements 2014). Many genera in Laeliinae can be crossed artificially (van den Berg et al. 2000, 2009). Many orchids are exquisitely adapted to individual pollinators whose sensory biases they may exploit (Schiestl 2010; Ramírez et al. 2011), but even here individual species of orchid bees, for example, may pollinate several species of orchids (N. H. Williams 1982), plant-pollinator relationships being highly nested; furthermore, few of the fragrances sought by male bees are unique to the orchids (Ramírez et al. 2011). Indeed, plant-pollinator specificity in euglossine orchid bees is lowest (from the bee's point of view) when a bee species is common and lowest (from the plant's point of view) when its flowering season is long, and seems to have little to do with in some way reducing extinction risk as by reducing dependence on unreliable pollinators - specificity is more apparent than real and is in part a matter of sampling (Ackerman & Roubik 2012).
However, pollinator specificity in orchids can be overemphasized. A single species of Epipactis may be visited by over 100 species of pollinators (Tremblay 1992), while in another study, pollinator specificity in orchids, although greater than that in Ranunculaceae (but that hardly says much), was less than that in Polemoniaceae (Waser et al. 1996). Geography may be connected with this. Southern African orchids have more specialized pollination systems than their European-North American counterparts, and in the latter there are fewer orchids pollinated by only a single species of pollinator (Ollerton et al. 2006). Cozzolino et al. (2004) found that in sympatric species pairs of Mediterranean orchids, if pollinators were shared, then post-zygotic cytological barriers tended to develop, but these barriers were not evident when the species had different pollinators. In European orchids with generalized food-deceptive mating mechanisms, barriers to crossing may be postzygotic, whereas those that practice sexual deception have prezygotic reproductive barriers, and introgression is more likely in this latter situation (Cozzolino & Scopece 2008).
Given the timing of evolution of orchids and bees, and the relative dependency relationships of the two, recent work strongly suggests that strict insect-orchid co-speciation is unlikely to be an important explanation for orchid diversification (e.g. N. H. Williams 1982; Szentesi 2002; Jersáková et al. 2006; Ramírez et al. 2011; Karremans & Díaz-Morales 2019). That the generation of diversity by floral specialization is relatively uncommon in flowering plants in general, although perhaps occurring in orchids (Armbruster & Muchhala 2009), is not inconsistent with this argument. Furthermore, factors other than floral variation may have contributed to orchid diversification - see also below" and "Ecology & Physiology" above.
Recent studies suggest that when pollinators visit orchid flowers in the course of deceptive pollination or to pick up scent rewards - specialized pollination mechanisms - pollinator specificity is greater and species richness is greater than when pollinators visit for nectar (Schiestl & Schlüter 2009; Xu et al. 2011; Schiestl 2012: sister-group comparisons; see also Dressler 1968; Scopece et al. 2010a for pollination efficiency). Thus deceit pollination may under certain situations increase outcrossing and speciation, the latter perhaps because of the specificity of the pheromones produced by the plants (Jersáková et al. 2006; see also Ledford 2007). However, this does not necessarily mean that there has been coevolution/cospeciation (Karremans & Díaz-Morales 2019).
The minute dust seeds of most orchids are a distinctive feature of the family (e.g. Moles et al. 2005a). They are often produced in huge numbers, up to 4,000,000 seeds per fruit or 74,000,000 seeds per plant, and are tiny, being 150 µm long or less (Arditti & Ghani 2000; Yam et al. 2009). Orchidaceae have particularly small seeds when compared with their immediate relatives (Moles et al. 2005a), and they usually lack endosperm (Clements, in Pridgeon et al. 1999 was unclear how common double fertilisation was here) and the embryo is undifferentiated. Much of the seed, small as it is, is in fact empty space ("air space"), estimates of this space being (16 - Pogonia-)43-93(-98 - Gymnadenia)%, and so orchid seeds are well suited for wind dispersal (Arditti & Ghani 2000). Fan et al. (2019) found that air spaces tended to be larger in terrestrial than in epiphytic orchids (terrestrial orchids including ex-epiphytic orchids that had become secondarily terrestrial), seeds with large air spaces tending to fall more slowly, so enhancing their dispersal, particularly important in terrestrial orchids where seeds are dispersed relatively close to the ground. The trichomes on the endocarp quite commonly found in Orchidaceae may function as elaters aiding in seed dispersal (Kodahl et al. 2015) while the hook-like structures on the seeds of Vandeae (Gamarra et al. 2018), for example, may be little grapnels aiding attachment to the bark.
The subterrananean mycoheterotroph Rhizanthella has baccate fruits with relatively few, large, crustose seeds (Weston et al. 2011), and in another mycoheterotroph, Yoania amagiensis, similar seeds are dispersed by camel crickets (Rhaphidophoridae: Tachycines elegantissima) (Suetsugu et al. 2017). Seeds of Apostasioideae are rather larger than those of other orchids, and those of A. nipponica, at least, have a lignified exotesta and are dispersed by endozoochory by crickets and camel crickets (Suetsugu 2020b, q.v. for other records). In Vanilla imperialis a white foamy substance exudes from the fruit, carrying the seeds along with it (Kodahl et al. 2015); indeed, Rodolphe et al. (2011) suggest that seeds in Vanilla, which are not winged and have quite thick-walled cells, may be dispersed by euglossine bees. Indeed, Lubinsky et al. (2006) noted that a number of genera in the three basal clades of orchids had aromatic fruits and might be dispersed by orchid bees, which might be the ancestrral condition fior the family...
Plant-Animal Interactions. Orchidaceae are not often eaten by caterpillars (Janz & Nylin 1998) or by insect herbivores in general, although Riodininae-Riodininae larvae may be found on them (Hall 2003 and references).
Coryanthes - the individuals are rather short-lived - is always to be found growing in ant gardens, and the plant has numerous extrafloral necatries, even on the flower buds. However, details of how the association develops are unclear (Gerlach 2017).
For pyrrolizidine alkaloids, scattered here, and homospermidine synthase (HSS), an early gene in the pathway that produces them that has evolved in the same way in other pyrrolizidine alkaloid-producing plants, see Nurhayati et al. (2009), Langel et al. (2010) and Livschulz et al. (2018a). The HSS gene has diverged considerably from the deoxyhypusine gene, from which it is derived, and Nurhayati et al. (2009) suggested that this was evidence of an ancient separation, although they were not sure where/when this happened. Pyrrolizidine alkaloids occur in genera like Phalaenopsis and Pleurothallis (see also Nurhayati et al. 2009) and are known to be involved in the defence of plants against herbivory, but the alkaloids are also sequestered by some herbivores for their own defence.
Bacterial/Fungal Associations. Orchids characteristically have very close associations with basidiomycete and some ascomycete fungi, but not with glomeromycotes (Imhof et al. 2013). Yukawa et al. (2009) suggested that Cantharellales (basidiomycetes), may have been the fungi first associated with Orchidaceae. The commonest families of fungi involved with orchids pretty much throughout the family are Tulasnellaceae, perhaps the most important (Martos et al. 2012), Ceratobasidiaceae and Serendipitaceae (see Currah et al. 1997 and Yukawa et al. 2009 for lists of fungi; Otero et al. 2002; Roy & Selosse 2009; Weiß et al. 2009, 2013). Some neotropical Epidendroideae have the basidiomycete Atractiellomycetes (in the same clade as Puccinia) as mycobionts (Kottke et al. 2010), and Sebacinaceae and ECM basidiomycetes are other partners (Weiß et al. 2016). (Note that the genus Rhizoctonia that is often mentioned in older literature is a common anamorph or form genus that encompasses a multitude of sins (Dearnalay et al. 2012), thus both basidiomycetes, e.g. Ceratobasidiaceae, Sebacinales-Serendipitaceae and Tulasnellaceae (Weiß et al. 2016), and ascomycetes, e.g.Tuber (Pezizales) (Setaro et al. 2012, 2013), have a Rhizoctonia stage.)
Rinaldi et al. (2008) thought that only 10 species of fungi might be involved in fungus-orchid associations. However, the number is far greater, even on a single species of orchid and in a relatively small area (e.g. Martos et al. 2012; Jacquemyn et al. 2013), while Duffy et al. (2019) found 75 species of orchid mycorrhizal fungi associated with Spiranthes spiralis sampled from a number of locations along a transect over 3,000 km long, diversity decreasing with increasing latitude. Overall, van der Heijden et al. (2015a) estimated that about 25,000 species of basidiomycete fungi alone were involved in associations with orchids, as many as in the mycorrhizal associations of all other embryophytes combined.
At least some saprophytic fungi living on decaying plant material also form close relationships with orchids (Ogura-Tsujita et al. 2009; Yukawa et al. 2009; Lee et al. 2015; Bayman et al. 2016). Such fungi are quite commonly associated with tropical mycoheterotrophic orchids (parasitic fungi may also be involved), although not in temperate species, however, ECM fungi, either forming quite specific or more generalized associations, are known from tropical mycoheterotrophic Neottieae (Roy et al. 2009), and this is discussed further above.
The fungi associated with the plant as it germinates may be quite different from those associated with the adult plant (e.g. Hashimoto et al. 2012; Rasmussen et al. 2015; Y.-I. Lee et al. 2015; Bayman et al. 2016). A variety of fungi, among which "Rhizoctonia" is important, form the initial fungus-orchid association, later on, specificity may be higher (Roy et al. 2009; Hynson et al. 2013; Rasmussen & Rasmussen 2014). For reasons that are not understood, Serendipitaceae (near-basal Agaricomycetes-Sebacinales), not ECM but saprophytic and endophytic, are important in seedling but not adult mycoheterotrophy, while Sebacinaceae, often ECM, may be found on adult but not seedling mycoheterotrophic orchids and their relatives (Weiß et al. 2016); see also Y.-I. Lee et al. (2015), Rasmussen et al. (2015 and references) and Bayman et al. (2016) for changes in partners, which also occurs in Ericaceae-Pyroloideae, and Whigham et al. (2008) for change, change = addition of partners, or no change at all. Interestingly, one effect of burning an orchid habitat may be a change in the fungus associated with an orchid. Thus in Victoria, Australia, before the burning Tulasnella calospora was found in quadrats along with the orchid Pterostylis revoluta, but afterwards Ceratobasidium was the fungus - and the orchids were not flowering (Jasinge et al. 2018). See Martos et al. (2012) for the literature on the phylogenetic signal of orchid and fungus, also above for the specificity of the fungus-orchid association.
The relationship between fungus and orchid is certainly not one-on-one (e.g. Roy et al. 2009; Martos et al. 2012: identification method important; Leake & Cameron 2012; Jacquemyn et al. 2013) and can even seem pretty random, at least in the ECM pezizalean associates (Tuber: ascomycetes) of Epipactis studied by Tesitelova et al. (2012). Shefferson et al. (2005, 2010) found rather narrow host breadth in fungi associated with Cypripedium and Goodyera respectively, which they thought was common in Orchidaceae and might be thought of as phylogenetic conservatism (Shefferson et al. 2010), but a close/narrow association does not convert to a unique association from the funguses point of view. Some orchids do have a wider suite of associates, indeed, there is variation in this within Cypripedium, which also has nice examples of orchid—fungal associations switching (Shefferson et al. 2007). Individual North American clades in the mycoheterotroph Corallorhiza striata complex (Epidendroideae-Maxillariinae) are associated with different sets of the fungus Tomentella (Thelephoraceae: Barrett et al. 2010), and Bidartondo et al. (2004) discussed potential host specifity in several European orchids. Roche et al. (2010) studied the specificity of the Tulasnella-Chiloglottis association (see also Otero et al. 2011: Pterostylinae).
Overall, orchid fungal networks are not nested, that is, specialist fungi, forming associations with only a few species of orchids, are only rarely also found on generalist orchids growing in the same area - fungi in these latter also grow on other generalist orchids (in this orchid mycorrhizae are like ECM and ericoid mycorrhizal associations - Toju et al. 2016 and references). However, recent work on orchids growing on Réunion suggests that the nature of the mycorrhizal network in epiphytic and terrestrial orchids differed there, with only 10 of the 95 fungal species (= taxonomic units) recorded being found in members of both groups of orchids, fungal associations were nested in epiphytic orchids (most species of Angraecum) and specificity was higher there. Furthermore, most of the fungal species, whether restricted to one of the groups or occuring in both, were found on only one or two orchid species (Martos et al. 2012). Differences between the species of fungi found in the two habitats, or in features of the orchids that affect colonization by the fungi, may both explain this striking pattern (Leake & Cameron 2012).
Chomicki et al. (2014b) discussed the association of the root-photosynthetic and epiphytic orchid Dendrophylax with endomycorrhizal fungi. Plant-fungal relationships are discussed further above; see also Jacquemyn and Merckx (2019), etc..
Recent work by Ghirardo et al. (2020) has documented the extensive metabolomic changes in both fungus and plant at the protocorm stage in the association between the agaric Tulasnella calospora and Serapias vomeracea (Orchidoideae-Orchideae). Interestingly, a variety of lipids were to be found in the fungal mycelium growing outside the protocorms while there were chito-oligosaccharides in the protocorms themselves.
For endophytic fungi, see Bayman and Otero (2006). Very little is known about them, and the one fungus may even be both pathogen, endophyte, and mycorrhizal symbiont.
Vegetative Variation. Orchidaceae show considerable diversity in habit and other vegetative features despite their generally modest size. However, some Sobralieae are slender, cane-like plants up to about 10 m tall, while viny Vanilloideae, including the mycoheterotrophic Galeola [= Erthyrochis] altissima, may be several metres long. The geophytic habit is quite common in Orchidoideae in particular. Stems, leaves and even roots may be succulent (Nyffeler and Eggli 2010b; also Figueroa et al. 2008: see above). Leaves are variously arranged (but not opposite), and may be terete or isobifacial, while individual leaf blades of taxa like Bulbophyllum fletcherianum may be up to 2 m long, some 15 cm across and about 5 mm thick (B. minutissimum, on the other hand, is 3-4 mm tall). Tatarenko (2007) summarized the extensive vegetative variation of temperate orchids, i.e. especially Orchidoideae.
The roots of mature plants of "leafless" Epidendroideae-Vandeae and those of many other Epidendroideae appear to lack root hairs, although they may develop on the side of the root facing the substrate (von Guttenberg 1968; Pridgeon 1987). Bernal et al. ((2015) report distinctive spiral thickenings on root hairs of some Orchidoideae-Spiranthinae), the hairs being described as a continuation of the velamen, and they are interspersed among other root hairs - which also look rather distinctive. The vegetative body of some of these epiphytic Epidendroideae-Vandeae consists largely of photosynthetic roots. These roots may be stout (ca 5 mm across) and terete, as in Dendrophylax, while those of the aptly named Taeniophyllum are distinctively flattened (e.g. Carlsward et al. 2006b: see also above). Inflorescences and flowers are more normal, although the bracts would seem to carry out little in the way of photosynthesis.
Moreira and Isaias (2008) found that the terrestrial orchids they examined had thicker roots than did the epiphytic orchids, but the latter do often have very thick roots as can readily be seen when walking around the orchid houses at MoBot. In epiphytic orchids in particular a velamen, made up of dead cells with spiral thickenings on the cell walls, is well developed around the outside (von Guttenberg 1968; see below). Pneumathodes are common in Epidendroideae. Leafless Vandeae have aeration units, distinctive exodermal cells, a space beneath, and a pair of thin-walled cortical cells in their roots; such aeration units are also found in related leafy Vandeae (Benzing et al. 1983; Carlsward et al. 2006a, b). Roots of New World epiphytic Epidendroideae in particular have distinctive tilosomes, cells of the innermost layer of the velamen that are adjacent to the passage cells of the exodermis and that have complex often lignified excrescences developing from the wall (Pridgeon 1987; Pridgeon et al. 1983; Porembski & Barthlott 1988). However, such cells are also found in ground-dwelling Orchidoideae-Spiranthinae (Figueroa et al. 2008) and their exact function is unclear.
The vernation of orchid leaves varies, being flat to plicate. The blade may be quite thin to very thick, bifacial, isobifacial or unifacial (terete), and the leaf base is sometimes massively swollen (Bulbophyllum). Leaves may be spirally arranged to 2-ranked, and are sometimes deciduous, being articulated with the sheathing base (common in Epidendroideae). Some ground- and shade-dwelling species have distinctively-coloured and -patterned leaves - variegated, purple-mottles, two surfaces of different colours (e.g. Bone et al. 2015b: variegation = absence of chlorophyll?) - that makes them particularly attractive to horticulturists. Extrafloral nectaries are scattered, for instance being found on the stems opposite the leaves in Vanilla and at the bases of the pedicels in Cymbidium.
The End. We can now return to the question, Why are there so many species of orchids? As noted above, diversification may have increased in Orchidaceae (108.8-)73.1(-59.7) Ma (Magallón et al. 2018), and the family is distinctive in several ways, of which their flowers and fruits - inverted/resupinate, monosymmetric flowers with a column and labellum, and minute, endospermless seeds - are just two. However, these are pretty much common throughout the family and are unlikely to be the immediate causes of major diversification given the sizes of the basal clades (see next paragraph), although they form the basis of the subsequent radiation of the family (Givnish et al. 2015). Vegetative and physiological variation, more or less associated with habit and habitat, is almost equally striking, and features of the core Epidendroideae such as shifts to the epiphytic habit and perhaps the adoption of CAM photosynthesis (see above, are as likely to have been as important in orchid diversification as anything else (Gravendeel et al. 2004; Givnish et al. 2015). Indeed, one could argue that it is the highly speciose and commonly epiphytic (some CAM) core Epidendroideae with their eight or so tribes and around 18,850 species (figures from Pridgeon et al. 2005, 2009, 2014), about two thirds of the entire family, that are distinctive (e.g. Freudenstein & Chase 2015). The main clades of core Epidendroideae may have diverged from each other only 37.9-30.8 Ma (rather older in G.-Q. Zhang et al. 2017), and diversification rates for the clade as a whole and even more so for some clades within it are notably high (Givnish et al. 2015, 2016a: c.f. stem age of subfamily, 2018).
A number of other features, most not immediately associated with core Epidendroideae, may also have contributed to this increased diversification.
- Waterman et al. (2011) distinguish between speciation and coexistence in orchids, and note that shifts in details of pollination (placement of pollinaria, pollinating insect) occur with speciation of the orchid, although associations with different fungi may promote the coexistence/co-occurrence of immediately unrelated orchid species.
- A genome duplication is thought to have shortly preceded the origin of crown-group Orchidaceae ca 81 Ma (G.-Q. Zhang et al. 2017: Asparagus the only out-group, huge error bars), however, Zwaenepoel and Van de Peer (2020) question the existence of this event.
- Epidendroideae in particular are diverse in montane habitats in New Guinea, South America, etc., and the geography/topograhy of such areas may have facilitated speciation (Givnish et al. 2015; see also Rhododendron), and in both the Old (Bulbophyllinae) and New (Pleurothallidinae) Worlds there are very large clades in which fly/deceit pollination is prevalent (see above). Note, however, that differences in the topology when nuclear and chloroplast phylogenies are compared may affect where on the tree acquisition of deceit pollination is to be placed (Pérez-Escobar et al. 2020/2021). Givnish et al. (2016a) discuss the biogeography and diversification rates of the family in some detail, emphasizing the role that long distance dispersal has played, and also the importance of the evolution of pollinia, the epiphytic habit and invasion of the northern Andes by the pleurothallid orchids. Indeed, the Andean uplift and current great Andean diversity stand in a similar relationship to neotropical diversity as a whole - no uplift, no exceptional neotropical diversity (Gentry 1982).
- Cozzolino and Widmer (2005; see also Schiestl 2005) suggested that orchid diversification is associated with the mimicry/deceptive pollination mechanisms that are so prevalent in the family.
But to return to a point made earlier, looking at the numbers of species of orchids and of particular clades within the family is just one way to approach the problem. One cannot think about orchid diversification without also thinking about the evolution of the whole [Asparagales + commelinid] clade. Putting the numbers above in this broader context suggests that orchids are perhaps less diverse than advertised. Orchidaceae, with around 27,800 species, are indeed a very speciose family, but of course the family rank is meaningless in such comparisons, and sister-group relationships within the [Asparagales + commelinid] clade allow one to see the problem in a somewhat different light. Orchidaceae are sister to the rest of Asparagales, which have ca 7,100 species, far fewer than Orchidaceae but nevertheless an appreciable number (c.f. Sargent 2004: Orchidaceae compared with Hypoxidaceae - only 100-220 species). Continuing the numbers game, Asparagales as a whole, with around 32,900 species, are sister to commelinids, which have some 24,500 species - not that different. And as we have seen, within Orchidaceae, clades of 14, 245, and 170 species are successively sister to the rest, so also suggesting a rather more complicated story (Givnish et al. 2015; see also in part S. A. Smith et al. 2011; P. Soltis et al. 2019), and this would be emphazed by the placement of Petrosaviales as sister to Orchidaceae (see H. T. Li et al. 2019). Indeed, Orchidaceae with their distinctive flowers show similar phylogenetic/diversity patterns as do angiosperms with their distinctive flowers, and numbers alone may suggest no immediate connection between flowers and success.
Of course, Orchidaceae have long been recognised as a family because they are florally, at least, all rather similar in some ways, indeed, floral variation in the family at one level can be thought of as being a series of remarkably intricate variations on a rather limited theme (see also Mondragón-Palomino 2013 and below). Most species have a single anther, a labellum, a very similar gynoecium, etc., with variation centred on the pollinaria and labellum, so another way of looking at the problem is to think of causes for their conservatism. Other Asparagales, although they have only about one third the species, could perhaps be considered vegetatively and even florally more diverse than Orchidaceae, and that is why they have been placed in a number of families, and the same is even more true of the commelinids. Of course, it is very hard to make such comparisons, and Burleigh et al. (2006) suggest that by some measures Orchidaceae do show a notable increase in complexity. The bottom line is that answers to a question like "Are orchids particularly diverse, and if so, why?", are not straightforward, but for several variations of this question, the answer is simply "no".
Genes & Genomes. For a possible genome duplication in the common ancestor of Orchidaceae, see G.-Q. Zhang et al. (2017, q.v. for the Apostasia shenzhenica genome) and references. The VAPLα event, some 119.7 Ma, can be linked with the [Vanilloideae [Cypripedioideae [Orchidoideae + Epidendroideae]]] clade (Landis et al. 2018: ?Cyp).
Chromosome number and size vary considerably. Thus Apostasioideae, Epidendroideae and Orchidoideae have small chromosomes, while larger chromosomes occur in Cypripedioideae and Vanilloideae. Felix and Guerra (2010) survey chromosome number variation in Epidendroideae and I. de Oliveira et al. (2015) that in Pleurothallidinae; Epidendreae as a whole may be x = 20. Faminhão et al. (2021) discuss the extensive variation in chromosome numbers in the Epidendroideae-Vandeae-Angraecum group where i.a. there seems to have been a shift n = 17, 18 → 25, that number being unique in the subfamily; there has been substantial ascending and descending dysploidy, etc., here although chromosome number changes are not associated with shifts in diversification rates.
For genome sizes, which vary 168-fold, see Chase et al. (2005: epiphytic Oncidiinae), Leitch et al. (2009), Jersáková et al. (2013), Yin et al. (2016) and Moraes et al. (2017: the largest genomes in Maxillariinae arise in different ways).
The rate of molecular evolution in the plastome is notably high in Orchidaceae when compared with that of other Asparagales (Barrett et al. 2015b). MatK in Apostasioideae may be in transition from a possibly functional gene to a pseudogene; in other Orchidaceae examined (but the sampling is poor) it is a pseudogene (Kocyan et al. 2004). There have been three or four losses of ndh genes, and details of the loss of nuclear transcripts encoding NDH proteins vary (Ruhlman et al. 2015); more detailed sampling is needed to work out what is going on. Indeed, Y.-K. Kim et al. (2019) looked at chloroplast genomes across the family, and found that all 11 ndh genes were lost/pseudogenized in the 10 species of Aeridinae they examined (and in a few other Epidendroideae).
Wicke et al. (2016), Graham et al. (2017), Lallemand et al. (2019) and others have looked at the overall picture of changes in the plastid genome that are associated with the adoption of mixotrophy and mycoheterotrophy. The plastid genome of the subterranean mycoheterotroph Rhizanthella (Orchidoideae-Diuridae) is very small, about 59 kbp, but there is still a core group of functioning genes (Delannoy et al. 2011), and over two dozen functional genes were found in the still smaller genome of Epipogium, to 19 kbp (E. roseum), the particular genes that remained functional depended on which essential genes had moved to the nucleus, etc. (Schelkunov et al. 2015). Barrett and Davis (2012), Barrett et al. (2014a, b, 2018) and Z.-H. Li et al. (2020) discuss the gradual degeneration of the chloroplast genome in mycoheterotrophs in Calypsoinae with a focus on plastome degradation in Corallorhiza; there the amount of the plastome retained is about proportional to how much photosynthesis is going on in the plant and pseudogenization and gene loss in the chloroplast can be extensive. Thus Li et al. (2020) found that the plastome of Danxiaorchis zingchiana to 26/27 housekeeping genes and the three photosynthesis-related genes, while that of Risleya atropurpurea had only 25 housekeeping genes; Barrett and Kennedy (2018) also discuss genome size in the parasite-autotroph continuum. In Hexalectris there are four to five transitions to mycoheterotrophy and with (infraspecific) variation in genes lost, etc., and in one accession of H. arizonica the IR has been lost (Barrett et al. 2019b). Several small inversions occur in the plastomes of Vandeae-Aeridinae (Y.-K. Kim et al. 2019). For more on plastome evolution, see also Dong et al. (2018) and Wicke and Naumann (2018).
Sinn and Barrett (2019) discuss mitochondrial gene transfer from a smut fungus, Ustilago, to orchids. There was a small-scale primary transfer probably in the ancestor of all orchids, and a secondary and far larger transfer that replaced the first; the latter is so far known only from Epidendroideae, although what is going on in Orchidoideae and Cypripedioideae is unknown (Sinn & Barrett 2019).
Chemistry, Morphology, etc.. For lignin with catechyl units, see F. Chen et al. (2012).
Porembski and Barthlott (1988) describe the root velamen and its systematic significance; there is some doubt as to whether or not Apostasioideae have a velamen, and here I follow Pridgeon (1987). Furthermore, Porembski and Barthlott (1988) noted that all Apostasioideae, also a number of Orchidoideae, Cypripedioideae, etc., had a rhizodermis, but Pridgeon (1987) scored only the single Apostasioideae he examined and no other orchid as having a simple epidermis; one might have thought that a rhizodermis and a simple epidermis were the same thing... Orchidaceae are one of the few non-commelinid clades with SiO2 bodies, and here they are born in stegmata, cells immediately adjacent to sclerenchymatous tissue (e.g. Prychid et al. 2003b); the silca bodies show some variation in form and are sometimes lost (Freudenstein & Rasmussen 1999). Paphiopedilum, but not other Cypripedioideae, lack chloroplasts in stomatal guard cells (D'Amelio & Zeiger 1988: other oddities in the family).
Cardoso-Gustavson et al. (2014; see also Bogarín et al. 2018) discuss the occurrence of bicellular hairs ("colleters") that often secrete mucilage in the flowers of Epidendroideae. They note that these may be on the outside of the flower, and suggest they may be connected with the extrafloral nectaries on the inflorescences of some Epidendroideae.
Incumbent anthers are recorded from many orchids, especially Epidendroideae, where incumbency is of two type. Anthers can be bent forwards by column elongation quite late in development, or by very early anther bending, the latter in vandoids; a third way in which anthers become incumbent occurs in Vanilloideae, and there cells of the anther connective elongate considerably (e.g. Kurzweil 1987; Freudenstein et al. 2002; Valencia-Nieto et al. 2018). In Epidendreae, anthers became incumbent early in Calypsoinae, late in other subtribes. Anthers of some species appear to be bisporangiate in early development (Freudenstein & Rasmussen 1996). At least some Orchidaceae have placentoids (Weberling 1989). There seems to be some uncertainty over gynoecial construction. The capsule often has 6 "valves", and authors like Vermuelen (1966) suggested that the gynoecium was six-carpelate. However, there are only three (or fewer) stigmatic lobes, and Kurzweil (1999), for example, thought that there were only three carpels, the outer three of the six valves being made up of the midveins of the carpels and surrounding tissue, the other three consisting of the adjacent halves of neighbouring carpels with a placenta in the middle. Rasmussen and Johansen (2006), suggested that these outer three valves represented tissue of the outer tepals that separated when the capsule was mature, and they are the sterile valves of Mosquera-Mosquera et al. (2019). Although most Orchidaceae have capsular fruits dehiscing laterally, the fruits of Apostasioideae are variable. Most are either baccate or basically just fall to bits, but the fruits of Nieuwiedia veratrifolia are septicidal, the valves falling off, but rib-like structures in the position of the outer three valves just mentioned persist (see de Vogel 1969). I have placed this character as a family-level apomorphy, but there are alternative ways of treating it. Prutch and Schill (2000) discuss variation in the morphology and ultrastructure of the stigma; variation seems to be at about the subfamilial level. Kodahl et al. (2015) discuss embryo sac formation (6-nucleate embryo sacs are common in the family), double fertilization (extent unclear) and endosperm development (or lack thereof); see also Swamy (1949a), Wirth and Withner (1959), Abe (1972a, b) and Duarte et al. (2019 and references) for the diversity of embryo sac development here. Although the seeds are generally minute and the testa cells have thin walls, Selenipedium (Cypripedioideae) has a hard, dark testa, although apparently it lacks phytomelan; seeds of Vanilloideae are notably variable (Cameron & Chase 1998).
For general information, the series of volumes edited by A. M. Pridgeon, P. J. Cribb, M. W. Chase and F. N. Rasmussen deserve special notice representing as they do the synthesis of just about all information available when they were written - for Apostasioideae and Cypripedioideae, see Pridgeon et al. (1999), for Vanilloideae, Pridgeon et al. (2003), for Orchidoideae, Pridgeon et al. (2001b, 2003), and for Epidendroideae, see Pridgeon et al. (2005, 2009, 2014), and see also Schlechter (1992, 1996, 2003), Dressler (1993), Szlachetko (1995) and Pridgeon (2014), and for accounts of Apostasioideae, see de Vogel (1969), Pridgeon et al. (1999) and Stern et al. (1993: anatomy), for Cypripedioideae, see Atwood (1984) and Koopowitz (2017: easy-to-read account of their evolution), for Epidendroideae-Malaxidinae, see Margonska et al. (2012), for terrestrial orchids, see Rasmussen (1999), for mycoheterotrophic taxa, see Merckx et al. (2013a), general, Imhof et al. (2013: roots, mycorrhizae), and Waterman et al. (2013: pollination), for an illustrated generic account, see Alrich and Higgins (2008), for Cattleya see articles in Renziana vol. 4 (2014) and for Dendrobium, see J. J. Wood (2014) and Schuiteman (2013). Also: Anatomy, general, see Stern (2014), for roots, see Moreira and Isaias (2008) and Siegel (2015), for Epidendroideae, see Stern et al. (2004), Stern and Carlsward (2006, 2009), and Morris et al. (1996: Dendrobium), Orchidoideae, see Stern (1997a, b), Stern et al. (1993b), and Andreota et al. (2015: Cranichideae), Smidt et al. (2013: New World Bulbophyllum) and Avi and Rodrigues (2018: Pleurothallidinae), Vanilloideae, see Cameron and Dickison (1998: reticulate leaf venation), and for Apostasioideae, see Stern et al. (1993a). See also Pridgeon et al. (1983: tilosomes), Rasmussen (1987: stomata), Prychid et al. (2004: SiO2 bodies), Mayer et al. (2011: colleters, uncommon), Aybeke (2012: rhizome and roots of Orchidoideae and Epidendroideae, Limodorum rhizome with a ring of phloem surrounding a ring of xylem?).
In addition: Hirmer (1920), Kurzweil (esp. 1987a, b, 1988, 1993, 1998: useful summary), Endress (1994b), Kristiansen et al. (2001), Cameron (2002), Kocyan and Endress (2001a), Johansen and Frederiksen (2002), Kurzweil and Kocyan (2002), Bateman et al. (2013) and Royer et al. (2020: homologies in some complex Oncidiinae), all floral morphology and development, Bell et al. (2009: nectar spurs in Orchidoideae), Swamy (1948a: floral vasculature), Rao (1973: floral anatomy), Franken et al. (2016: osmophores), Valencia-Nieto et al. (2016: anther development, Epidendreae). For pollen morphology, see Newton and Williams (1978: Cypripedioideae, Apostasioideae), Schill and Pfeiffer (1977: general), Ackerman and Williams (1980: Neottieae), Zavada (1990 and references: general), P. Li et al. (2012: pollinia in Cypripedioideae), also Freudenstein (1991: endothecium), Clements (1995: embryology, etc.), Carlson (1945) and Yeung and Law (1997), embryology, Kurzweil (2000), Molvray et al. (2000), Cameron and Chase (2000), Szlachetko and Rutkowski (2000) and Szlachetko and Mytnik-Ejsmont (2009 and references), all gynostemium, the papers by Szlachetko alone involving ca 1,250 pages, Yeung (2005: embryogeny), Rasmussen and Johansen (2006: fruits), Gamarra et al. (2012: seed morphology and classification) and Barthlott et al. (2014: general seed survey).
Phylogeny. Cameron (2007) provided a summary of phylogenetic work on the family. With the advent of molecular studies, it was quite soon clear that the then current subfamilial limits were going to need adjustment (e.g. Kores et al. 1997). Most recently Sánchez et al. (2021) looked at variation in 78 plastid coding genes in 117 genera distributed between all subfamilies, 18 tribes and 28 subtribes; although around 67 genera are included in the nuclear analyses of Baker et al. (2021: see Seed Plant Tree) less can be said about relationships, although there seem to be few if any major conflicts with the tree based on the plastome data just mentioned.
There was initially some uncertainty over the position of Cypripedioideae (e.g. Cameron 2004), and in some analyses they grouped (albeit weakly) with Vanilloideae (Freudenstein & Chase 2001) or were sister to Orchidaceae minus Apostasioideae, which might make sense if thinking about androecial evolution alone (Cameron et al. 1999: one gene, successive weighting). However, they are usually placed sister to Orchidaceae minus Apostasioideae and Vanilloideae (e.g. Kocyan et al. 2004; Cameron & Chase 2000; Cameron 2002, 2005b, 2006: two genes, in a basal tritomy with atp alone; Górniak et al. 2010: nuclear gene Xdh; Givnish et al. 2015; Y.-K. Kim et al. 2019: plastomes; Serna-Sánchez et al. 2021: 78 plastome genes for 117 genera, all subfamilies, 18 tribes; etc.). This latter hypothesis, followed here, suggests that the monandrous condition may have evolved twice (see also Freudenstein et al. 2002, 2004). There are also suggestions that Codonorchis is sister to [Epidendroideae + Orchidoideae] (e.g. Clements et al. 2002) or basal in Orchidoideae (Cameron 2006: it has whorled leaves; c.f. Jones et al. 2002); the genus was sister to one of the two major clades that made up Orchidoideae in Givnish et al. (2015; see also Serna-Sánchez et al. 2021). In an analysis of chloroplast genomes, Dong et al. (2018) suggested that Orchidoideae were paraphyletic, but genera like Listera and Epipactis which they included in their Orchidoideae are basal in Epidendroideae here. Perez-Escobar et al. (2020/2021: Angiosperms353 nuclear analyses) obtained the same relationships that are recognized above in their nuclear analyses (294 genes, 89 taxa); all subfamilies were monophyletic. The position of Vanilloideae seemed uncertain in the nuclear analysis of Baker et al. (2021: see Seed Plant Tree); sister to Cypripedioideae perhaps remains a possibility.
For phylogenies of Apostasioideae, see Kocyan et al. (2004) and Yin et al. (2016).
Relationships within Vanilloideae are now fairly well resolved (Cameron 2004, 2009; Cameron & Molina 2006; Pansarin et al. 2008; Cameron & van den Berg 2017). Included are Pogoniinae (Erythrorchis, a mycoheterotroph, is here), Vanillinae, and Galeolinae and Lecanorchidinae (both mycoheterotrophs). Pansarin et al. (2012) evaluated the phylogeny of Pogonieae; Pogoniopsis is to be placed in Epidendroideae. Bouetard et al. (2010) provide a phylogeny for Vanilla.
For relationships in Cypripedioideae, including also a morphological survey, see Albert (1994). Commonly-retrieved relationships are [Cypripedium [Selenipedium [Paphipedium [Mexipedium + Phragmipedium]]]] (Guo et al. 2012; Koopowitz 2017). J.-h. Li et al. (2011) found that morphology sometimes had misled over relationships in Cypripedium; for a phylogeny of Paphiopedilum, see Chochai et al. (2012).
Orchidoideae include the erstwhile Spiranthoideae, the latter having incumbent anthers (as in Epidendroideae) with apical rostellar tissue; Spiranthes et al. are now placed in Cranichideae. Relationships within Orchidoideae are becoming fairly well resolved (e.g. Cameron 2004; see also Inda et al. 2010: cox1 intron; Givnish et al. 2015). Four tribes can perhaps be recognizrd [[Cranichideae + Diurideae] [Codonorchideae + Orchideae]] (Serna-Sánchez et al. 2021). For the phylogeny of Cranichideae, see Salazar et al. (2003: monophyly and characters of subtribes), while Górniak et al. (2006) and Salazar et al. (2011a, 2016) discuss relationships in Spiranthinae, most frequent in the Neotropics; Salazar et al. (2018, see also 2019) found that Cotylolabium lutzii was sister to the rest of the subtribe. Cisternas et al. (2012) discuss relationships in the American Chloraeinae. Salazar et al. (2011a) examined relationships around Dichromanthus et al. where adaptation to bird pollination has occurred in parallel, confusing generic limits, while Dueck et al. (2014) focussed on Spiranthes and its distribution. For relationships in Pterostylis and relatives (Pterostylidinae), see Clements et al. (2011). For relationships in Orchideae, see Bateman et al. (1997), Pridgeon et al. 1997), Inda et al. (2012) and Ngugi et al. (2020: the big picture). Raskoti et al. (2016) exmined relationships in Herminium and surrounds and Le Péchon et al. (2020) those in Holothrix. For relationships within Orchidinae and Habenariinae, see Bateman et al. (2003), Habenaria was polyphyletic and Orchis triphyletic (the other bits go in Anacampseros and Neottia). In Asia Habenaria is diphyletic and Platanthera triphyletic (Jin et al. 2014), the former problem being confirmed by Jin et al. (2017) in their study of Orchidinae. New World species of Habenaria are monophyletic, although sectional limits need revision (Batista et al. 2013; Pedron et al. 2014). Y. Tang et al. (2015) found a certain amount of conflict between nuclear and chloroplast data, and current genera of East Asian Orchidinae did not map well onto the clades that they were finding. Bateman et al. (2018b) emphasized the conflict between the relationships suggested by molecules and morphology in the [Dactylorhiza + Gymnadenium] area; these genera are close and also hybridize to a certain extent. Satyrium is sister to other Orchidinae (Jin et al. 2017). For relationships in the African Disa (Disinae), see S. D. Johnson et al. (1998) and Bytebier et al. (2007); the genus is especially diverse in the Cape Region. For a phylogeny of Satyrium, see van der Niet and Linder (2008); it has diversified in the Fynbos region (Verboom et al. 2009). Prescottiinae s.l. have diversified at very high altitudes - up to 4,900 m - in the Andes (Álvarez-Molina & Cameron 2009). Clemens et al. (2002; see also Miller & Clements 2014; Weston et al. 2014) clarify relationships of Diurideae, a few of which are to be placed in Epidendroideae; for information about relationships in the speciose Caladenia, see Australian J. Bot. 57(4). 2009, also Brown and Brockman (2015) for literature. For Codonorchis (Codonorchideae), see above.
For general phylogenetic relationships in Epidendroideae, see van den Berg (2005), Górniak et al. (2010) and especially Freudenstein and Chase (2015), Givnish et al. (2015) and Serna-Sánchez et al. (2021). Support for branching positions along the spine of Epidendroideae remains rather weak (e.g. Cameron et al. 1997; Pridgeon et al. 2001b; Cameron 2004), although less so in Givnish et al. (2016a). Neottieae, a clade of terrestrial orchids, are sister to all other Epidendroideae (Rothacker & Freudenstein 2006; Freudenstein & Chase 2015; Y.-K. Kim et al. 2019). X.-G. Xiang et al. (2012; see also Freudenstein 2012) found at least three more clades, including Sobralia and Elleanthus, Nervilia, and Tropidia respectively, to be successively sister to the rest at the base of the "higher", "upper" or "core" epidendroids. These taxa were all in a single clade in some analyses of Freudenstein and Chase (2015), while Triphora formed another clade; Nervilieae and Tropidieae formed a single clade in Givnish et al. (2015), as did Triphoreae and Sobralieae. Perez-Escobar et al. (2020/2021: nuclear loci) found relationships along the lines of [Neottieae [Xerorchideae [Gastrodieae [Nervilieae (nodes up to here usually with rather poor support) [Tropidieae (the last two sister taxa?) ...]]]]], while relationships in Serna-Sánchez et al. (2021) are along the lines of [Sobralieae, Triphoreae, Tropideae, Nervilieae (the last three perhaps a clade) [Arethuseae ...]]. These basal taxa/clades tend to lack articulated leaves, their pollinia are sectile/mealy (Pridgeon et al. 2005), and many are ground-dwelling plants and so their roots have no velamen. If their position is confirmed, this will affect identification of apomorphies for the subfamily and also for the highly speciose core Epidendroideae.
Relationships in Neottieae have been much studied. Palmorchis is sister to other members of the tribe (T. Zhou & Jin 2018; Lallemand et al. 2019). However, relationships between these other genera are rather unclear, branch lengths being very short (Feng et al. 2016; c.f. Lallemand et al. 2019 and references), although the genera do appear to be monophyletic.
Core Epidendroideae contain eight or so tribes (Freudenstein & Chase 2015; Givnish et al. 2015). In the plastome analysis of Y.-K. Kim et al. (2019: 31 species included), relationships recovered above the basal clades just mentioned were [Arethuseae [Malaxideae [Collabieae [Vandeae [Cymbidieae + Epidendreae]]]]], with strong support. Perez-Escobar et al. (2020/2021) obtained similar relationships in some of their nuclear analyses, although the relationships between the last three tribes were unclear and some genera there moved around - thus the positions of Coelia and Earina at the base of Epidendreae are uncertain, and in chloroplast analyses relationships between the last three subfamilies were [Epidendreae [Cymbidieae + Vandeae]]. In the chloroplast analyses of Serna-Sánchez et al. (2021) core epidendroid relationships are similar - [Arethuseae [Malaxideae [[Podochileae + Collabieae] [Epidendreae [Cymbidieae + Vandeae]]]]].
For relationships in the Calanthe group (Collabieae), with plicate leaves and also largely terrestrial, see Zhai et al. (2014). For Sobralieae, see Neubig et al. (2011). Malaxis and Liparis (Malaxideae-Malaxidinae), both with terrestrial species in temperate as well as tropical regions, may not be monophyletic, but are closely intertwined (e.g. Cameron 2005a; Margonska et al. 2012; L. Li et al. 2020). Calypsoinae is another basal group that includes largely temperate and terrestrial taxa (see Freudenstein et al. 2017 for a phylogeny). Within Malaxideae-Dendrobiinae, the speciose Dendrobium and many of its sections are turning out to be polyphyletic (Yukawa & Uehara 1996: vegetatively variable, florally perhaps less so; Yukawa et al. 1993, 1996, 2000; Clements 2003: ITS study, see also earlier work; Adams 2011: esp. Australian taxa; X.-G. Xiang et al. 2013); Xiang et al. (2016) recovered a split between an Australasian clade and an Asian-Malesian clade. Bulbophyllum is relatively little studied, but see Gravendeel et al. (2004), Smidt et al. (2011) and B. Gravendeel, E. de C. Smidt, G. Fischer & J. J. Vermuelen in Pridgeon et al. 2014; Fischer et al. (2007) studied the Malagasy species, Hosseini et al. (2016) those from Peninsula Malaya and A.-Q. Hu et al. (2019) taxa of the Cirrhopetalum alliance with their subumbellate inflorescences and twisted and ± connate lateral outer tepals. For diversification in Arethuseae-Coelogyninae, see Gravendeel et al. (2005), Freudenstein et al. (2017), Z.-H. Li et al. (2020) and others; Corallorhiza and Oreorchis are interdigitated (Li et al. 2020). For relationships around Hexalectris, see Sosa et al. (2016) and Barrett et al. (2019b). Pedersen et al. (2020) discuss relationships within Dendrochilum, where they found that D. pallidiflavens was sister to the rest of the genus. Zhang et al. (2013) discuss relationships in Calypsoeae. For relationships in Catasetinae, see Pérez-Escobar et al. (2015, 2017b). For studies in Cymbidieae, see M.-H. Li et al. (2016: general, relationships [Cymbidiinae [Cyrtopodiinae + The Rest]], support in the middle part of the tree rather weak), Serna-Sánchez et al. (2021), Yukawa et al. (2002: Cymbidium), Whitten et al. (2005: Zygopetalinae), Neubig et al. (2008: Dichaea, Zygopetalinae), Cieslicka (2006), Martos et al. (2014) and Bone et al. (2015a, b), all Eulophia and relatives (Eulophiinae), and Chase (1987), Chase and Palmer (1997), N. H. Williams et al. (2001a, b, 2005), Chase et al. (2009) and especially Neubig et al. (2012a), all focussing on Oncidiinae and the polyphyletic Oncidium, while Szlachetko et al. (2019) suggest that Wulfenia be dismembered. For a major study of Epidendreae-Pleurothallidinae, see Pridgeon et al. (2001b); Pleurothallis is not monophyletic (also Chiron et al. 2012: focus on Brazilian species) nor is Trichosalpinx (Bogarín et al. 2018). Serna-Sánchez et al. (2021: plastome data) also discuss relationships in Pleurothallidinae in some detail. Abele et al. (2005) and Matuszkiewicz and Tukallo (2006) discussed the phylogeny of Masdevallia, Karremans et al. (2012) examined relationships in Stelis, which has been extended to include "a few hundred" species of Pleurothallis (see Karremans 2019) and Karremans et al. (2016a) looked at Specklinia and its immediate relatives. For phylogenetic relationships in Laeliinae, see van den Berg et al. (2000), while Encyclia was studied by Leopardi-Verde et al. (2016), who found conflict between phylogenetic signals from ITS and chloroplast genes. Nuclear and plastid DNA also give conflicting signals in Cattleya (van den Berg 2015; see also Renziana 4. 2014). Epidendrinae: Pinheiro and Cozzolino (2013) summarize what is known about Epidendrum itself. Sosa et al. (2016; see also Sosa 2007) discuss relationships within the terrestrial (and some mycoheterorophic) Bletiinae. For Epidendreae see also Kulak et al. (2006). For studies in Maxillarieae, see Whitten et al. (2000), N. H. Williams and Whitten (2003), Sitko et al. (2006), Arévalo and Cameron (2013), and especially Whitten et al. (2007: Maxillaria to be restricted, generic realignments needed). Ng et al. (2018) looked at relationships in Podochileae. Russell et al. (2010) discuss phylogeny in the widely-distributed Polystachya (Vandeae-Polystachyineae: monopodial), where there is some correlation of polyploidy with broad species distributions. Topik et al. (2005) investigated relationships in Aeridinae; characters conventionally used to establish relationships showed little congruence with the tree they obtained (see also Hidayat et al. 2005; Zou et al. 2015); for relationships in and around Vanda itself, see Gardiner et al. (2013). For angraecoid orchids (Angraecinae) in general, see Stewart et al. (2006) and in particular Faminhão et al. (2021). Szlachetko et al. (2013: ITS), also Micheneau et al. (2008) and Andriananjamanantsoa et al. (2016), both esp. Madagascan taxa, as well as Simo-Droissart et al. (2018) looked at relationships around Angraecum; the genus itself and just about all its sections were polyphyletic (see also Martos et al. 2018). Within Angraecinae, there has been one shift to the New World, the ancestor of [Campylocentrum + Dendrophylax moving there (via the Antilles) within the last 10 Ma or so (Pessoa et al. 2018).
Classification. Chase et al. (2015; c.f. Chase et al. 2003) provide a higher-level phylogenetic classification for the family with practically all genera placed into subfamilies and tribes (see also World Checklist of Monocots). For genera and synonymy in Apostasioideae, see Pridgeon et al. (1999), Cypripedioideae, Pridgeon et al. (1999), Vanilloideae, Pridgeon et al. (2003), Orchidoideae, Pridgeon et al. (2001b, 2003), and in Epidendroideae, Pridgeon et al. (2005, 2009, 2014). Ngugi et al. (2020) suggest the division of Orchideae into nine subtribes.
Generic limits in the family are in the middle of a major overhaul to make them consistent with molecular findings, many of which have implications for clade/generic circumscriptions. Disagreements over generic circumscriptions in part reflect fundamental differences in classificatory philosophies and differing beliefs in the ability of morphology when used alone alone to disclose relationships. In the past the importance of floral differences in separating genera was emphasized, but here, as elsewhere, there has been widespread homoplasy in floral features (e.g. Chase et al. 2009 and references), for example, the distinctive lip-like appendage that was a defining feature of the old Corycinae (Waterman et al. 2009) seems to have evolved in parallel. Szlachetko et al. (2005 and references) give a statement of the "floral" position, maintaining that variation in column form, etc., yields taxonomically important characters (see also Szlachetko 1995; Rutkowski et al. 2008). However, clade limits suggested by molecular studies and generic limits suggested by floral features alone by no means always agree (Kocyan et al. 2008 and references). The features characterising the erstwhile broadly-delimited and polyphyletic Oncidium - mimicry of oil flowers of Malpighiaceae, whether or not the orchid itself also offers oil as a reward - is a good example of this (N. H. Williams et al. 2001; Neubig et al. 2008, esp. 2012a; Stpiczynaska & Davies 2008; Chase et al. 2009), similarly, in Aeridinae there is also probably widespread parallelism in the floral characters used to delimit genera (Hidayat et al. 2005; Salazar et al. 2011a, b for other examples). It is not that floral morphology is inherently taxonomically useless, but undue reliance on it may well lead us seriously astray if our interest is in understanding relationships. Indeed, in some Epidendroideae vegetative variation may correlate better with clades evident in molecular phylogenies (e.g. Cameron 2005a), although anatomical variation by itself may suggest little major phylogenetic structure (Stern et al. 2004; Stern & Carlsward 2006).
However, even having a phylogeny and agreeing over basic taxonomic philosophy does not lead to automatic agreement about generic boundaries. Thus Clements (2003, 2006) suggested a wholesale pulverization and reorganization of generic limits in Dendrobium and its relatives, placing them in some 50 genera in three subtribes. The species numbers given above do not reflect this, Burke et al. (2008), Janes and Duretto (2010), Schuiteman and Adams (2011), Schuiteman (2012, see also 2013: New Guinea) and X.-G. Xiang et al. (2013) all suggesting that a broader circumscription of the genus would be preferable; species limits are also at issue here (Adams 2011: focus on Australia). Jones and Clements (2002a, esp. 2002b) divide Pterostylis, Clements et al. (2011) noting that there are nine or so identifiable groups around there, although that may not be quite the point - all identifiable groups do not have to be called genera. Since the monophyly of Pterostylis s.l. has been confirmed, its division is questionable (if one likes broadly-drawn generic limits), and indeed Janes and Duretto (2010) and Jones et al. (2010) suggest returning to the old circumscription of the genus (see also Clements in Chase et al. 2015). Jones et al. (2001) also dismember the monophyletic Caladenia and Clements et al. (2002) divide a monophyletic Corybas, as do Jones et al. (2002 - also much else). Such cases simply reflect conflicting preferences for narrow or broad genus limits, so they are something of a pain. In any event, in Australia, the result of nomenclatural changes made for these and other reasons is that about 45% of the species and subspecies in the entire orchid flora acquired new generic names between 2000 and mid-2009 (Hopper 2009). Finally, Reveal (2012) came up with an earlier name for Epidendroideae (10 versus 58,500 hits - Google search iv.2012), although it seems to have returned to blessed obscurity.
There have been extensive discussions about generic limits in European Orchidinae in which many of the issues concerning classification in the context of phylogenies have been raised (e.g. Bateman et al. 1997; Bateman 2001, 2009, 2012; Tyteca & Klein 2008, 2009; Scopece et al. 2010b; M. Kropf in Kadereit et al. 2016). In an attempt to make generic limits there more objective, Scopece et al. (2010b) found that clade membership correlated well with post-zygotic reproductive isolation (embryo death). A phylogeny-based classification in which this and other evidence was incorporated could, they thought, be defended on more explicit grounds, and this would allow morphologically distinctive taxa previously segregated as separate genera be incorporated into their proper clades (Scopece et al. 2010b). This approach is somewhat reminiscent of that of Danser (1929), and although perhaps useful in Orchidaceae - but it is going to be interesting to see how widely it can be applied even here, and what the taxonomic consequences are - it may be inapplicable to orchids with different breeding behaviours. For an account of Anacamptis, Orchis, etc., see Kretzschmar et al. (2007). Pace (2020) looked at generic limits around Goodyera (Cranichideae).
For generic limits in Maxillariinae, c.f. Whitten et al. (2007) and Szlachetko et al. (2012). Schuiteman and Chase (2015) adopted a broad circumscription for Maxillaria, interestingly, 19 of the 42 generic names they placed in synonymy had been described in the last ten years. For a reclassification of Pleurothallidinae, see Pridgeon and Chase (2001), although Pleurothallis may not be monophyletic, c.f. Karremans et al. (2012). Karremans et al. (2016a) discuss the synonymy of Specklinia. Karremans (2016) enumerated genera in Pleurothallidinae as a whole, Karremans et al. (2016b) provided an infrageneric classification of Acianthera, and Karremans (2019) provided an infrageneric classification for a somewhat broadly circumscribed Stelis, with some 1423 species, 1030 of which are in Stelis s. str., the largest genus of the subtribe. This is a huge group, and sampling is still relatively very poor. There is some controversy over generic limits in the Masdevallia area, c.f. Luer (2006) and Pridgeon (2007). Blanco et al. (2007) made many new combinations in genera of Maxillariinae. Ng et al. (2018) provide a classification for Podochileae. For generic limits around Angraecum, see e.g. Szlachetko et al. (2013) and Simo-Droissart et al. (2018); for those around Cattleya, see van den Berg (2014) and articles in Renziana vol. 4 (2014), including an infrageneric classification; for those around Bulbophyllum, see Pridgeon et al. (2014) and Vermuelen et al. (2014); while for an infrageneric classification of Vanilla, see Soto Arenas and Cribb (2010). Generic limits in Habenariinae are discussed by Batista et al. (2013 and references) while Y. Tang et al. (2015: pp. 22-24; see also Jin et al. 2017) include an interesting discussion about generic limits around the polyphyletic Amitostigma (Orchidinae) - they end up with a broadly circumscribed Hemipilia. Further changes are in the offing, as is clear from the discussion in Chase et al. (2015), especially in genera like Angraecum (a broad circumcription is adopted in the generic list), Habenaria, Coelogyne, etc.. Indeed, in the Angraecum group, as sampling of both taxa and genes improves, relationships change, and the limits of genera proposed five years before are modified (Simo-Droissart et al. 2018), while Faminhão et al. (2021) used phylocods-type names to talk about particular clades within the group.
I do not pretend to have dealt with hybridization in Orchidaceae satisfactorily, in particular hybridization by horticulturalists. Those interested should consult Sander's list of registered hybrids (Royal Horticultural Society 2008, also see the quarterly updates by the Society ("Quarterly Supplement to the International Register and Checklist of Orchid Hybrids (Sander's List)". Generic name changes can have considerable consequences here. Thus the acceptance of generic name changes in some Epidendroideae in Pridgeon et al. (2005) necessitated over 10,000 changes to the names of hybrids which had to be transferred to a hybrid genus other than the one in which they were originally registered (Royal Horticultural Society 2008). It is a relief that names of hybrid genera can have no more that eight syllables, so Sophrolaeliocattleya gets in just under the wire.
The final issue has to do with species numbers, numbers that depend both on the general state of our knowledge of orchid diversity and more particularly on issues of how to draw species limits - not totally unconnected, of course. As to our general knowledge of orchid diversity, Karremans and Davin (2017) summarize the rate of publication in Pleurothallidinae since the publication of Luer's Icones pleurothallidinarum beginning in 1975, a rate that has held constant over the ensuing 40+ years at around 85-90 new and accepted species/year. There are over 8,000 published names of which over 3,550 are currently accepted, and Luer was the sole or joint author of 2,634 names during this period (Karremans & Davin 2017). The rate of publication of novelties shows no signs of abating, and Karremans and Davin (2017) estimate that by 2026 there will be close to 6,000 accepted species in the subtribe, up from around 1,650 in 1975. As to species limits, here is just one example already mentioned, but by no means unique: Are there 16 or 252 species of Ophrys (Bateman et al. 2006a, esp. 2011a, 2018a; Devey et al. 2008; Bradshaw et al. 2010; Vereecken et al. 2011; Alibertis 2015: photographs of the species/"species")?
[[Boryaceae et al.] [[Ixoliriaceae + Tecophilaeaceae] [Doryanthaceae [Iridaceae [Xeronemaceae [Asphodelaceae [Amaryllidaceae + Asparagaceae]]]]]]]: (monocot secondary thickening +); (stem fructans +); (cuticular waxes as platelets transversely arranged in parallel series); (T ± connate), (trichomes at apex); (A inserted on T tube); tapetal cells bi- to tetranucleate; seeds exotestal.
Age. This node is dated to around (97-)89(-79) or 85.1 Ma (S. Chen et al. 2013), about 102.9 Ma (Magallón et al. 2015), and about 119 Ma (Tank et al. 2015: Table S2).
Evolution: Divergence & Distribution. I have put the character "outer tepals with apical trichomes" - they may be papillae or hairs, they vary in their exact position, etc. - here, although it is not flagged as an apomorphy. This feature has recently been studied in some detail, and presence or absence of these trichomes seems to vary at quite a high level, although if an apomorphy, it has been lost several times; the trichomes are involved in holding the tepals together in bud (Macfarlane & Conran 2017 for details of this character and its distribution).
Vegetative Variation. Monocot secondary thickening, a distinctive pattern of secondary growth, is scattered in this clade (e.g. see list in Carlquist 2012a), where it has evolved perhaps ten times, and it has also been reported from Eriocaulaceae and Rapateaceae (Poales: Scatena et al. 2005). A meristem cuts off tissue primarily to the inside, and vascular bundles embedded in ground tissue differentiate in it, some tissue may be cut off to the outside (Tomlinson 1970; Tomlinson & Zimmermann 1969; Zimmermann & Tomlinson 1972; Rudall 1991, 1995b; Jura-Morawiec et al. 2021). It can perhaps be thought of as the continued activity of the primary thickening meristem (see also Cheadle 1937; Carlquist 2012a), although there is some discussion as to what exactly that is (see above). There is sometimes a transition from collateral to amphivasal vascular bundles as the secondary thickening phase takes over, but this is by no means always so (e.g. Diggle & DeMason 1983; Rudall 1984). There are complex patterns of branching and fusion of the vascular bundles of the stems and branches (Haushahn et al. 2014), and Mangin (1882) had suggested there might be a connection between the origin of this secondary thickening and the reticulum of vascular bundles in association with which lateral roots arise in monocot stems. In monocots genes involved in secondary thickening via a normal bifacial cambium have been lost and reacquisiition of the woody habit has involved the evolution of novel mechanisms of secondary thickening (Davin et al. 2016; Roodt et al. 2019), although Zinkgraf et al. (2017) suggested that some of the genetic mechanisms involved in the regulation of ordinary secondary thickening had become reactivated here. Jura-Morawiec et al. (2021: table 2, Asphodelaceae, Asparagaceae studied) discuss the differences between monocot vascular cambia and those in other angiosperms - in the former, the cambial cells are of a single type, they are much shorter, there is no intrusive growth, etc.. Of course, palms and bamboos in particular have become woody without developing secondary thickening.
Chemistry, Morphology, etc.. For the distribution of fructose oligosaccharides, see Pollard (1982) and Meier and Reid (1982). Although recorded there only for some Hypoxidaceae in the [Boryaceae [Blandfordiaceae [Lanariaceae [Asteliaceae + Hypoxidaceae]]]] clade, and not for some of the smaller families elsewhere in Asparagales, fructans seem to be widespread in this part of the tree; they were not recorded from Orchidaceae.
[Boryaceae [Blandfordiaceae [Asteliaceae [Lanariaceae + Hypoxidaceae]]]]: septal nectaries external; ovules with hypostase; embryo sac with chalazal constriction, antipodal cells persistent.
Age. This node can be dated around (87-)67(-47) or 42/65.2 Ma (S. Chen et al. 2013: last two numbers should be the same - c.f. Table 3), Ma (Janssen & Bremer 2004: but c.f. topology) or ca 93.3 Ma (Magallón et al. 2015).
There are many dates for clades in this area in both Janssen and Bremer (2004) and Wikström et al. (2001), but the topologies there differ from that above; if relationships change, some ages may be of use.
Evolution: Divergence & Distribution. There is extensive homoplasy in this little clade, so exactly where features like "septal nectaries external" are to be placed is unclear.
Chemistry, Morphology, etc.. For some information, see Kocyan and Birch (2011).
Phylogeny. The [Blandfordiaceae [Lanariaceae [Asteliaceae + Hypoxidaceae]]] clade is an at most moderately well-supported - if consistently appearing - group (Rudall et al. 1998a; Chase et al. 2000a; Fay et al. 2000; Davis et al. 2004 - Lanariaceae not included; Graham et al. 2006; Chase et al. 2006; etc.). Relationships between Milligania (Asteliaceae), Lanaria and Blandfordia were suggested by Bayer et al. (1998a). Kocyan and Birch (2011: all genera studied) found that Lanariaceae, Asteliaceae and Hypoxidaceae formed a tritomy, while Seberg et al. (2012) found that jackknife support for the clade was poor, and that Asteliaceae and Lanariaceae reversed their positions, i.e. to [Asteliaceae [Lanariaceae + Hypoxidaceae]], and relationships were also scrambled in Janssen and Bremer (2004) and Wikström et al. (2001).
BORYACEAE M. W. Chase, Rudall & Conran - Back to Asparagales
Plant xeromorphic, (growth monopodial - Alania), (aerial pseudostems +), rhizome often short, (with stilt roots); roots mycorrhizal, velamen + [?all], raphides 0; (monocot secondary thickening - Borya); endodermis much thickened; vascular bundles with lateral phloem; leaves spiral, base sheathing; inflorescence scapose, involucrate, capitate; T tube short; A adnate to tube [not Alania]; anthers (centrifixed), little longer than wide; septal nectaries external; micropyle bistomal, parietal tissue 1 cell across; T persistent in fruit; (seed papillate - Borya); endosperm without starch, embryo short, ovoid; n = 11, 14, x 7 (?6, ?8); seedling?
2 [list]/12. Australia, scattered (map: see Brittan et al. 1987). [Photo - Borya Habit © M. Fagg]
Age. Crown group Boryaceae are dated to 54 Ma (Janssen & Bremer 2004).
Evolution: Ecology & Physiology. The arborescent Borya can tolerate extreme dessication, but with some interesting wrinkles - the response is facultative in some species, or only a small part of the leaf may be dessication tolerant (e.g. Barthlott 2006; Gaff & Oliver 2013 and references). The plant is poikilochlorophyllous (the chloroplasts ± break down on drying), and the leaves can remain living but completely dessicated for four years or so (e.g. references in Gaff 1981).
Bacterial/Fungal Associations. Borya has tuberculate roots that may have the coil-forming Rhizoctonia fungus in them (c.f. Orchidaceae).
Chemistry, Morphology, etc.. The stems of Borya have monocot-type secondary thickening (Porembski & Barthlott 2000). There are vessels with almost simple perforation plates in the stem (Carlquist 2012a). The pedicels of Alania have several bracteoles.
Additional information is taken from Dahlgren et al. (1985) and Conran (1998), both general, Gaff (1981 and references), anatomy/physiology, Porembski and Barthlott (2000), velamen, and Conran and Temby (2000), floral morphology.
Previous Relationships. Genera of Boryaceae have often been included in Anthericaceae (= Asparagaceae-Agavoideae), as by Takhtajan (1997).
[Blandfordiaceae [Asteliaceae [Lanariaceae + Hypoxidaceae]]]: ?raphides; leaf blade with distinct midrib; nucellar cap ca 2 cells across.
Age. The age of this clade is estimated at (98-)81, 74(-56)Ma by Bell et al. (2010: note topology), at (79-)58(-35) or ca 38.3Ma by S. Chen et al. (2013), and about 84.5 Ma by Magallón et al. (2015).
Chemistry, Morphology, etc.. See Conran and Temby (2000) for general information, especially about ovules.
BLANDFORDIACEAE R. Dahlgren & Clifford - Back to Asparagales
Rhizome short; chemistry?; velamen +; plant glabrous; leaves two-ranked, vernation flat-curved, sheath?; inflorescence a raceme; pedicels articulated; T large, tubular; (A adnate below middle of tube), anthers latrorse, centrifixed; pollen trichotomosulcate; G stipitate, septal nectaries external; style short, stigma ± punctate, dry; outer integument 3-4 cells across, hypostase +; capsule septicidal; exotesta papillate; embryo short; n = 17, 27, x = ?; cotyledon photosynthetic.
1 [list]/4. E. Australia (map: see Brittan et al. 1987). [Photo - Blandfordia Flower © B. Walters.]
Age. The age of this clade was estimated at (7-)4(-1.5)Ma by S. Chen et al. (2013).
Evolution: Divergence & Distribution. Hardly a terribly diverse clade (Tank et al. 2015: Table S1).
Chemistry, Morphology, etc.. Information is taken from Clifford and Conran (1998: general), Di Fulvio and Cave (1965) and Prakash and Ramsey (2000: both embryology) and Kocyan and Endress (2001b: some floral morphology.
Previous Relationships. Rudall (2003a) suggested that there was a close morphological relationship between Boryaceae and Blandfordiaceae.
[Asteliaceae [Lanariaceae + Hypoxidaceae]]: plants ± rosette-forming or caespitose; hairs multicellular, often branched; stomata paracytic; G ± inferior, septal nectaries internal; ovule with bistomal micropyle, micropyle zig-zag.
ASTELIACEAE Dumortier - Back to Asparagales
Plant ± rhizomatous; saponins +; indumentum branched-lepidote-stellate; leaves 3-ranked, linear, ensiform, or subulate, base sheathing, closed or open; plant dioecious (polygamodioecious/flowers perfect), inflorescence branched raceme or spike, inflorescence bracts large; flowers rather small, T connate basally (free) (10-14); staminate flowers: A (10-14), adnate to base of T/free; (nectaries on outside of ovary), pistillode +; pistillate flowers: staminodes +, G superior (subinferior), (5-7), (placentation parietal), intra-ovarian trichomes +, style branched or not (short), stigmas lobed-capitate to decurrent, dry; ?nucellar cap; fruit a berry; funicle distinct [= "long"], (with ± well developed mucilaginous hairs); endosperm oily, thin-walled, no hemicellulose, embryo "well developed"; n = 30, 35, ...105, x = ?, chromosomes 4-6 µm long; cotyledon not photosynthetic, ligule long, primary root well developed.
3 [list]/31 (37). Australia and New Zealand to New Guinea, Pacific Islands E. to Hawai'i,Chile, the Mascarenes (map: see van Steenis & van Balgooy 1966; Fl. Austral. 45. 1987). [Photos - Milligania & Astelia Flowers © C. Howells - Australian Plants Society, Tasmania.]
Age. Crown-group Asteliaceae are dated to ca 92 Ma (Janssen & Bremer 2004); Birch et al. (2012) date it to (76-)55.4(-36.0) Ma and S. Chen et al. (2013) 32.6 or (51-)29.5(-12.5) Ma, while (76-)53.8(-36) Ma is the estimate in Birch and Keeley (2013).
Fossils from New Zealand identified as stem-node Astelia are ca 23.2 Ma (Iles et al. 2015).
Evolution: Divergence & Distribution. Birch and Keeley (2013) provide numerous dates for clades within the family.
For the biogeography of Asteliaceae, see Birch et al. (2008, 2011, esp. 2012) and Birch and Keeley (2013). The initial divergence of Astelia may have been in New Zealand in the Oligocene at a time when the island may have been all or mostly under water... One species of Astelia is known from Réunion - it is older than the island (see also Rousseaceae, Arecaceae, Monimiaceae, etc.) - one from southern South America, etc.. Asteliaceae may have initially been Australian, but with subsequent very extensive long distance dispersal (Birch & Keeley 2013). For the Mascarenes/Africa-Hawaii/Antipodes connection, see also Malvaceae (Kokia), Asteraceae (Hesperomannia); Keeley and Funk (2011) give a list of Hawaiian endemics, also see Acacia (Fabaceae).
Given current ideas of relationships in the family (see below), character evolution in it will repay investigation.
Chemistry, Morphology, etc.. Carlquist (2012a) suggested that vessels were practically absent, except perhaps in the roots - although this might depend on the technique used to prepare the material.
For additional information, see Brittan et al. (1987) and Bayer et al. (1998a), both general, and Prakash and Ramsey (2000: embryology).
Phylogeny. The phylogeny of the family has been clarified by Birch et al. (2009); Milligania, with loculical capsular fruits, a semi-inferior ovary and no intra-ovarian trichomes, perfect flowers, etc., and often considered rather different from other Asteliaceae, seems to be embedded in Astelia, as do the other small genera previously recognized in the family (Birch et al. 2008, esp. 2009). However, Birch et al. (2012) and Birch and Keeley (2013) found the relationships [[Neoastelia [Milligania + Astelia]].
Classification. Astelia is to include Collospermum (Birch et al. 2012); for an infrageneric classification of the former, see Birch (2015).
[Lanariaceae + Hypoxidaceae]: ?
LANARIACEAE R. Dahlgren - Back to Asparagales
Plant with vertical rhizome; biflavones +; raphides 0, (styloids +); indumentum dendritic; leaves two-ranked to spiral, sheath ?closed; inflorescence branched; T connate half-way; A adnate in mouth of tube; style long, stigma small, subcapitate; ovules 2/carpel, apotropous, outer integument 5-7 cells across, parietal tissue ca 3 cells across, obturator +; capsule type?; seed 1; exotesta palisade, other cells rounded, tegmen persists, develops at micropyle; endosperm initially with starch, embryo medium; n = 18, x = ?; seedling?
1 [list]/1: Lanaria plumosa. Cape Province, South Africa. Photo: Habit, flower.
Evolution: Divergence & Distribution. There may have been a slowing of diversification in this clade (Hertweck et al. 2015, but c.f. topology).
Chemistry, Morphology, etc.. Information is taken from De Vos (1963) and Steinecke and Hamann (1989), both embryology, Dora and Edwards (1991 - chemistry) and Dahlgren (in Dahlgren & Van Wyk 1988) and Rudall (1998), both general.
HYPOXIDACEAE R. Brown, nom. cons. - Back to Asparagales
Stem ± cormose to rhizomatous, leaf bases persisting, contractile roots common; fructan sugars accumulated, saponins 0; velamen +, dimorphic root hypodermis 0; stomata (tetracytic), with oblique or parallel cell divisions; leaves 3-ranked, (with petiole and blade), (apex bilobed), vernation (conduplicate-)plicate (flat), (unifacial), sheaths also closed; inflorescence various, scapose, axis flattened; (flowers 2-merous); T free to long-tubular; (A inserted towards base), (many), (3, plus 3 staminodes adnate to style [= gynostemium] - Pauridia), (extrorse), (basi- or centrifixed, sagittate); tapetum amoeboid, microsporogenesis successive [tetrads tetragonal]; (pollen disulcate, trisulcate [Pauridia], inaperturate); (apical beak +), nectaries 0, (placentation parietal - Empodium), stigmas commissural, ± 3-radiate, dry or wet; ovules apotropous, (outer integument to 4 cells across), (nucellar cap 0), (parietal tissue 0); (embryo sac bisporic, 8-celled [Allium type]), antipodal cells soon die; fruit dehiscing laterally, loculicidal/(circumscissile)/dry, indehiscent/baccate, (with a long beak [= persistent corolla tube]); seeds globose, smooth to spiny, (strophiole +); exotesta palisade or not, (endotegmen persistent), raphe prominent; endosperm (nuclear), thin-walled, (perisperm +, slight), embryo short, ± undifferentiated; n = 6-11, x = 9, chromosomes 2-5 µm long, nuclear genome [1 C] (?0.125-)1.588(-?) pg; cotyledon not photosynthetic, ligule long.
7-9[list]/100-220 (159): Hypoxis (50-100), Pauridia (31). Seasonal tropics, esp. southern Africa (temperate) (map: see Fl. N. Am. 26: 2002; Australia's Virtual Herbarium xi.2012). [Photo - Inflorescence, Flower.]
Age. Crown group Hypoxidaceae have been dated to as much as ca 78 Ma (Janssen & Bremer 2004) and as little as (33-)23(-16) or ca 15.6Ma by S. Chen et al. (2013).
This is a rather small but quite variable and poorly understood family.
Evolution: Pollination Biology & Seed Dispersal. Pollen is the main reward, and flies of various kinds, beetles and bees seem to be the pollinators (Kocyan et al. 2011 for a summary; Ren et al. 2018). At least some species of Hypoxis are apomictic (Nordal 1998).
Chemistry, Morphology, etc.. Kocyan (2007) found that some flowers of Curculigo racemosa were polyandrous, however, the stamens were not fasciculate. The staminodes of Pauridia that are adnate to the style rather surprisingly appear to represent the outer androecial whorl - and they are responsible for reports of a 6-lobed stigma in the family. The rostrum, a narrowed, beak-like apical part of the ovary, appears to have evolved more than once, but its function is uncertain; a beak may also be formed by the connate tepals.
There is controversy over the tapetum type in the family and in the numbers of nuclei in the cells, and whether or not there is a velamen in the root. The ovules have a parietal cell, so are not tenuinucellate [?incorrect - not in the literature I have read]. The endosperm is reported as being nuclear or helobial; if the former, then the antipodal cells tend to persist (de Vos 1948, 1949).
Additional information is taken from Nordal (1998), Judd (2000) and Wiland-Szymanska (2009: east Africa), all general, Rudall et al. (1998a: anatomy), Thompson (1976: vegetative; 1978 floral morphology), Kocyan and Endress (2001b: floral morphology), Stenar (1925: embryology), and and Arekal (1967: ovule and seed).
Phylogeny. Kocyan et al. (2011) recovered three main clades - Curculigo et al., Pauridia et al., and Hypoxis - in the family, a slight modification of the results obtained by Rudall et al. (1998). Relationships between these clades was unclear.
Classification. For genera, see Kocyan et al. (2011) and Snijman and Kocyan (2013).
Previous Relationships. Rudall (2003a) suggested that there might be a close morphological relationship between Hypoxidaceae and Orchidaceae. In older classifications, Hypoxidaceae were often included in Amaryllidaceae.
[[Ixoliriaceae + Tecophilaeaceae] [Doryanthaceae [Iridaceae [Xeronemataceae [Asphodelaceae [Amaryllidaceae + Asparagaceae]]]]]]: ?
Age. The age of this node is estimated at ca 84 Ma by Eguiarte (1995), (98-)87, 78(-68) Ma by Bell et al. (2010), ca 80 Ma by S. Chen et al. (2013: Fig. 3), and around 89 and (88.9-)84.3(-80.7) Ma by Magallón et al. (2015 and 2018 respectively).
Evolution: Divergence & Distribution. Diversification may have increased at this node (Magallón et al. 2018).
[Ixioliriaceae + Tecophilaeaceae]: cormose; root pith 0; leaves spiral, shortly cylindrical at apex [Vorläuferspitze]; flowers quite large; outer T mucronate to aristate, T tube short; A inserted at mouth of tube; fruit a loculicidal capsule; embryo long; x = 12.
Age. For the age of this node, some (93-)79, 70(-59) Ma, see Bell et al. (2010), while (79.3-)64.1(-46.5) or ca 34.1 Ma is the estimate in S. Chen et al. (2013) and ca 79.7 Ma in Magallón et al. (2015). The divergence of Ixoliriaceae is dated to ca 112 Ma and that of Tecophilaeaceae to 108 Ma (Janssen & Bremer 2004: note topology).
Evolution: Divergence & Distribution. The rate of diversification may have slowed in this clade (Hertweck et al. 2015: all three).
Chemistry, Morphology, etc.. The outer tepals in at least some Iridaceae (and Orchidaceae!) are also mucronate to aristate.
Phylogeny. There is weak to moderate support for this taxon pair in Chase et al. (2000a), Pires et al. (2006), Givnish et al. (2006) and Seberg et al. (2012), and stronger support in Graham et al. (2006: sampling poor); they have a very long branch in the three-gene analysis of Fay et al. (2000). Davis et al. (2004) found some support for the clade [Ixoliriaceae + Iridaceae], although sampling was poor; Chase et al. (2006) found strong support for this relationship. Janssen and Bremer (2004) found the pectinate relationships [Ixoliriaceae [Tecophilaeaceae [Doryanthaceae + the rest]]], while the relationships [Tecophilaeaceae [Doryanthaceae [Ixoliriaceae + Iridaceae]] the rest] in Chase et al. (2006) had very little support.
Previous Relationships. Both Dahlgren et al. (1985) and Takhtajan (1997) recognised relationships between Ixoliriaceae and Tecophilaeaceae, as well as with a selection of other asparagalean families.
IXIOLIRIACEAE Nakai - Back to Asparagales
Plant a tunicated corm; saponins 0?; root dimorphic exodermis 0, peduncle with a sclerenchymatous ring; mucilage cells +; leaf base ?type; inflorescence subumbellate, leafy; A centrifixed; tapetal cells uninucleate; stigma 3-lobed, dry; outer integument 3-4 cells across, parietal tissue ca 2 cells across, nucellar cap ca 2 cells across; seeds angled, phytomelan +; endosperm walls pitted, starch in cells surrounding embryo; x = 6 (?8, ?7), nuclear genome [1 C] (0.096-)3.291(-112.341) pg; cotyledon remains white even when exposed to light!
1[list]/3. Egypt and Turkey to Central Asia and Pakistan (map: from Traub 1942, rather approximate). [Photo - Flower © A. Shoob]
Chemistry, Morphology, etc.. The vascular bundles in the leaf are unequal in size, some in the inflorescence axis are arranged in a circle, enclosing additional scattered bundles.
Information is taken from Kubitzki (1998b: general), Arroyo (1982) and Arroyo and Cutler (1984: both anatomy), Dönmez and Isik (2008: pollen), Stenar (1925: embryology), and Tillich (2003: seedling morphology).
Previous Relationships. The inflorescence axis is leafy, the flowers are blue and there are no alkaloids, all unusual features for Amaryllidaceae, where Ixiolirion has often been included (e.g. Takhtajan 1997).
TECOPHILAEACEAE Leybold, nom. cons. - Back to Asparagales
Corm, tunicated, (in vertical series), (tuber); ?saponins +, fructan sugars accumulated [Cyanastrum]; roots raphides 0; stomata variable; leaf with petiole and blade/linear, more than one order of parallel veins, (transverse veins branching, reticulated), sheaths closed (none); inflorescence a raceme, branched or not/flowers axillary; (bracteoles 0); flowers monosymmetric (polysymmetric); (T tube moderately long); A (strongly heteranthous)/(4-3, staminodes 2-3), anthers dehiscing ± by pores; tapetal cells binucleate; pollen operculate (not - Kabayea, Cyanastrum); ?nectary; G (semi-inferior; carpels free - Cyanastrum), stigma punctate; ovules 2-many/carpel, ana-campylotropous, micropyle bistomal, outer integument "thick", vascularized [Cyanastrum], parietal tissue 3-5- cells across, funicular obturator +; seed (one/fruit); phytomelan +/0, (0, surface warty, with tufts of small hairs), testa multilayered, (exotesta palisade), thick-walled; endosperm nuclear (helobial - Odontostomum), thick-walled, pitted or not, (± absent), ?starch (0), (chalazosperm + - Cyanastrum), embryo also short; n = 8, 10-12, 14, x = 12, chromosomes 2-4 µm long, nuclear genome [1 C] (0.074-)2.498(-84.385) pg; cotyledon not photosynthetic, (coleoptile +), primary root long (hypocotyl and primary root 0 - Cyanastrum).
7 [list]/25: Cyanella (9). Africa, Chile, and the U.S.A. (California - Odontostomum) Map: from Carter (1962), Scott (1991), Brummitt et al. (1998) and Fl. N. Am. 26 (2002). [Photo - Flower, Flower.]
Age. Crown-group Tecophilaeaceae have been dated at ca 87 Ma (Janssen & Bremer 2004), ca 77 Ma (Buerki et al. 2013a), and (41-)30(-20) or ca 20.4 Ma (S. Chen et al. 2013).
Evolution: Divergence & Distribution. Buerki et al. (2013a) discussed the complex eco-biogeographical history of this small clade, i.a. they noted that its colonization of what are now Mediterranean ecosystems occurred before the origin of the Mediterranean climate, as seems to be common (see also Vargas et al. 2014).
Pollination Biology & Seed Dispersal. The floral morphology of Tecophilaeaceae suggests buzz pollinations (see also Russel et al. 2015).
Chemistry, Morphology, etc.. This is a heterogeneous group. Cells adjacent to stomata in Cyanastrum were described as having parallel cell divisions by Tomlinson (1974).
The monosymmetry of the flower is largely caused by the androecium; enantiostyly also occurs in a few species of Cyanella. Odontostomum has been reported to have six staminodia alternating with the six stamens; the "staminodia" are some kind of corona or enation from the tepals.
Some information is taken from Dahlgren (in Dahlgren & van Wyk 1988), Rudall (1997), Simpson and Rudall (1998), Brummitt et al. (1998) and Manning and Goldblatt (2012); for some embryology, etc., see Nietsch (1941), Cave (1952) and A.-m. Lu et al. (1985: Tab. 1 - summary), and for seedlings, variable in morphology, see Tillich (1996a, 2003).
Phylogeny. Tecophilaea was found to be sister to the rest of the family, although with only moderate support; other relationships along the backbone were poorly resolved (Brummitt et al. 1998). More recently, Buerki et al. (2013a) found that the clade [Conanthera + Zephyra] (both genera are from South America) were sister to the rest of the family.
Classification. Given the poor support for many relationships here, a classification is premature (c.f. Brummitt et al. 1998); despite a more resolved phylogeny, Buerki et al. (2013a) quite reasonably elected not to develop any formal suprageneric hierarchy.
Synonymy: Androsynaceae Salisbury, Conantheraceae Pfeiffer, Cyanastraceae Engler, Cyanellaceae Salisbury, Walleriaceae Takhtajan
[Doryanthaceae [Iridaceae [Xeronemataceae [Asphodelaceae [Amaryllidaceae + Asparagaceae]]]]]: ?
Age. this node has been dated to ca 107 Ma (Janssen & Bremer 2004); the separation of Doryanthaceae from Iridaceae (sic) has been estimated at ca 82 Ma (Goldblatt et al. 2008).
Pollen fossils assigned to Iridaceae-Isophysis or to Doryanthes have been found in Late Cretaceous rocks ca 75-70 Ma old from Eastern Siberia (Hoffmann & Zetter 2010).
Phylogeny. There is only moderate support for this node in Fay et al. (2000) and practically no support in Seberg et al. (2012), but 92% bootstrap support in Graham et al. (2006: note sampling); see also Janssen and Bremer (2004).
DORYANTHACEAE R. Dahlgren & Clifford - Back to Asparagales
Huge sub-bulbous tufted perennial; steroidal saponins +; root cortex with fibres; stem vascular bundles encased in fibres; styloids +, raphides 0; cuticular wax rodlets parallel, stomata paracytic, subsidiary cells with oblique divisions; leaves spiral, apex cylindrical [= Vorläuferspitze], when older as dry threads; inflorescence with inflorescence bracts, (subumbellate); T large, with two rows of vascular bundles, apex [esp. of outer T] cucullate, tube long; (A also adnate to the base of the tepal lobes), anthers latrorse, centrifixed, endothecium thick; pollen trichotomosulcate, surface reticulate; G inferior, stigma 3-angled, punctate, dry; ovules in two ranks, outer integument ca 5 cells across, inner integument ca 2 cells across, parietal tissue ca 5 cells across, nucellar cap ca 2 cells across, suprachalazal tissue extensive, postament +; antipodal cells to 5, ± persistent; fruit dehiscing laterally, loculicidal; seeds flattened, winged; testa multiplicative, many-layered, with phlobaphene; endosperm thin-walled, embryo flattened; n = 17, 18, 22, 24, x = 6 (?8, ?7), karyotype bimodal, nuclear genome [1 C] (0.337-)3.134(-29.176) pg; seedling with laterally compressed haustorium, coleoptile +.
1 [list]/2. E. Australia. Map: from O. Seberg (pers. comm). [Photo - Habit.]
Age. The divergence of the two species in the family is estimated to have occurred (8-)4(-1) Ma (S. Chen et al. 2013).
Chemistry, Morphology, etc.. The genus is described as being monocarpic by Forster and Eggli (2020), although usually it is pleonanthic - i.e., all the rosettes making up the one genotype do not flower at once. Kocyan and Endress (2001b) note that the connective is massive, each stamen being supplied by 2-4 "vascular complexes", although these were not observed by Newman (1928, 1929). There may be a hypostase immediately beneath the embryo sac (Newman 1928).
General information is taken from Wunderlich (1950), Clifford (1998) and Forster and Eggli (2020), Blunden et al. (1973) described leaf anatomy and Tillich (2003) seedling morphology.
[Iridaceae [Xeronemataceae [Asphodelaceae [Amaryllidaceae + Asparagaceae]]]]: (vegetative fructans +); (seeds with glucomannans as reserves); Arabidopsis-type telomeres lost, (TTAGGG)n [human-type telomeres] common.
Age. This node is estimated at (92-)81, 72(-62) Ma by Bell et al. (2010), (83-)75(-65) or ca 51.2 Ma by S. Chen et al. (2013), about 80.7 Ma by Magallón et al. (2015), (93-)83.1(-73.4) Ma by Joyce et al. (2018), about 98.1 Ma by Tank et al. (2015: Table S2) and (68.0-)62.7(-58.0) Ma by D.-F. Xie et al. (2020).
Evolution: Divergence & Distribution. Givnish et al. (2018b) suggest that there has been an acceleration of speciation in this clade.
Genes & Genomes. The loss of Arabidopsis-type (A-type) telomeres is not simple; human-type telomeres ((TTAGGG)n) may predominate, but there are other types, too. Asparagaceae-Scilloideae agree with other members of this clade, although the A-type telomere is somewhat more common than in the other members sampled (Adams et al. 2001; especially Sýkorová et al. 2003b, 2006a, b). Acanthocarpus, alone among the taxa discussed there as being an out-group, also lacks A-type telomeres, but it belongs to Asparagaceae-Lomandroideae (ex Laxmanniaceae), so it is an ingroup, not Arecales-Dasypogonaceae, a commelinid.
Chemistry, Morphology, etc.. The plants may have distinctive carbohydrates (Meier & Reid 1982; Buckeridge et al. 2000a). Apparently there are only tracheids in the xylem (Fahn 1990).
Glucomannan seed reserves are scattered in this clade, being associated with thick-walled endospermal cells, but I do not know details of their distribution. They are reported from Iridaceae, Amaryllidaceae-Allioideae, Asparagaceae-Asparagoideae and -Scilloideae-Ornithogaleae - and they are also known from some Liliales (see e.g. Elfert 1894; Jakimow-Barras 1973; Reid 1985).
Phylogeny. This group has quite strong support in Fay et al. (2000) and Soltis et al. (2007a), etc., but lacking much jackknife support in Seberg et al. (2012: bootstrap support better).
IRIDACEAE Jussieu, nom. cons. - Back to Asparagales
Plant rhizomatous; roots mycorrhizal; flavone C-glycosides, flavonols +, chelidonic acid 0?; dimorphic root hypodermis +; (stem endodermis +); raphides 0, styloids +; cuticular wax rodlets parallel; leaves two-ranked, ventralized isobifacial [oriented edge on to the stem]; flowers usu. large; T ± free, apex often aristate; A 3, opposite outer T, extrorse, endothecial cells with U-shaped thickenings; G opposite outer T, septal nectary 0, style branched, stigma dry; micropyle endo- or exostomal, outer integument 4-6 cells across, parietal tissue 1(-2) cells across (absent); seed testal and tegmic, phytomelan 0, phlobaphene +, endotesta pigmented, with lipids; endosperm thick-walled, hemicellulosic, embryo quite large; x = 10 (?9, ?8), nuclear genome [1 C] (0.145-)3.014(-62.805); cotyledon not photosynthetic, (hypocotyl short).
66 [list, as subfamilies]/2,120 (2,244) - eight subfamilies below. World-wide (map: see Heywood 1978 [S. America], Hultén & Fries 1986; Mathew 1989; Fl. N. Am. 26: 2002; Bahali et al. 2004; FloraBase 2005; Davies et al. 2005: Fig. 2b suggests that Iridaceae grow throughout Africa, much of the Arabian Peninsula, etc.; Rodrigues & Sytsma 2006; Alexeyeva 2008). [Photos - Collection.]
Age. Crown group divergence is estimated to have begun ca 96 Ma (Janssen & Bremer 2004), (82.9-)71.6(-60.5) Ma (Joyce et al. (2018), 70 or 66 Ma (Goldblatt et al. 2008), or (68-)58.5(-49) or 51.2 Ma (S. Chen et al. 2013).
1. Isophysidoideae Thorne & Reveal
Vessel elements in roots with scalariform perforation plates; amentoflavone + [= biflavonoid]; crystals 0 [leaves]; flower solitary, with spathes; T spreading; endothecium with radially elongated walls; microsporogenesis?; ovary ± superior [P, A, adnate basally], style branches ± spiralling, commissural; endosperm ?helobial; n = ?; seedling?
1/1: Isophysis tasmanica. Tasmania.
Synonymy: Hewardiaceae Nakai, nom. illeg., Isophysidaceae F. A. Barkley
[Iridoideae [Patersonioideae [Geosiridoideae [Aristeoideae [Nivenioideae + Crocoideae]]]]]: xanthone + [mangiferin], fructan sugars accumulate; vessel elements in roots with scalariform and simple perforation plates; (vernation plicate); inflorescence with cymose units [flowers from the axils of successive prophylls, so they alternate = a rhipidium]; flowers short lived [open ca 1 day]; (pollen operculate [often with two exine bands in a sulcus]); (style branches bifid), stigma on the edges of the complex/expanded branches; ovules 1-many/carpel; endosperm nuclear.
Age. The age of this node is around 62 Ma (Goldblatt et al. 2008).
2. Iridoideae Eaton
(Plant bulbous); γ-glutamyl peptides, (steroidal saponins), (bufadienolides), meta carboxy aromatic amino acids +; vessel elements in root with simple perforation plates; (leaf vernation plicate); rhiphidia simple; flowers (long-lived), (monosymmetric); T whorls strongly differentiated; T nectaries +; endothecial cells with spiral thickenings; (pollen grains with encircling aperture); style branches long, tubular; seedling (with ligule or coleoptile - e.g. Tigridia); n = 6<.
Ca 30/890. Worldwide, but esp. the spine of Central and South America.
Age. The age of the clade is ca 57 Ma (Goldblatt et al. 2008).
2a. Diplarrheneae Goldblatt
Flowers monosymmetric; A 2; pollen grains spherical, inaperturate, intectate; septal nectaries +.
1/2. S.E. Australia, Tasmania.
[Irideae [Sisyrinchieae [Trimezieae + Tigridieae]]]: ?
2b. Irideae Kitt.
(Plant cormose); mangiferin + [= xanthone]; (inner whorl T bearded - some Iris); (filaments connate); ovules with nucellar cap, obturator from funicle/inner integument.
Iris (350), Moraea (200).
[Sisyrinchieae [Trimezieae + Tigridieae]]: (floral elaiophores + [trichomal])
2c. Sisyrinchieae Klatt
Vessels in stems and leaves; T whorls similar (differentiated); filaments ± connate; endothecial cells?; style branches commissural (style undivided, stigma capitate - Solenomelus); embryo photosynthetic.
6/205: Sisyrinchium (140-216). America, few in Australasia.
[Trimezieae + Tigridieae]: ?
2d. Trimezieae Ravenna
2e. Tigridieae Kitt.
mangiferin + [= xanthone].
[Patersonioideae [Geosiridoideae [Aristeoideae [Nivenioideae + Crocoideae]]]]: rhipidia 2, fused [binate], each unit with 2-many flowers; extra codon in rps4 gene.
Age. The age of this node is about 70 or 55 Ma (Goldblatt et al. 2008).
3. Patersonioideae Goldblatt
Plant ± woody and rhizomatous; amentoflavone + [= biflavonoid]; (monocot secondary thickening +); vessel elements in roots often with scalariform perforation plates; inner tepals reduced to scales or 0; endothecial cells with base-plate thickenings, filaments ± connate; pollen spherical, inaperturate, intectate; stigma lobes broad; ovules apparently uniseriate; embryo small; n = 11, 21; two extra codons in rps4 gene.
1/24. More or less open conditions, scattered in Malesia, New Caledonia, and the periphery of Australia (map: partly from Fl. Austral. 46. 1986).
[Geosiridoideae [Aristeoideae [Nivenioideae + Crocoideae]]]: ?
Age. This node is about 48 Ma (Goldblatt et al. 2008) or (64.5-)53.2(-42.2) Ma (Joyce et al. 2018).
4. Geosiridoideae Goldblatt & Manning
Plant echlorophyllous, mycoheterotrophic; crystals 0 [leaves]; leaves heterobifacial; flowers sessile; T connate basally only; microsporogenesis successive; (style swollen towards the apex, stigma truncate); ovules with outer integument 2-3 cells across, parietal tissue 1-2 cells across; seeds minute, dust-like, mesotesta 0; endosperm starchy, walls thick, hemicellulosic, embryo small; n = ?
1/3. Madagascar, the Comores (Mayotte I.), and Australia (Queensland), also the Philippines? (Joyce et al. 2018).
Age. Crown-group Geosiris is at least (43.9-)29.9(-16.1) Ma (Joyce et al. 2018).
Synonymy: Geosiridaceae Jonker
[Aristeoideae [Nivenioideae + Crocoideae]]: ?
Evolution: Divergence & Distribution. The age of this node is estimated to be around 40 Ma by Goldblatt et al. (2008) and (49-)34, 31(-17) Ma by Bell et al. (2010).
5. Aristeoideae Vines
Plumbagin + [= acetogenic naphthoquinone]; monocot secondary thickening +; vessel elements in roots often with scalariform perforation plates; leaf bundles embedded, marginal sclerenchyma 0; T connate basally only; outer integument 2-3 cells across [?all]; embryo small; n = 16.
1/55. More or less open conditions, sub-Saharan Africa and Madagascar.
[Nivenioideae + Crocoideae]: flowers long-lived; T connate; septal nectary +.
Age. The age of this node is ca 36 Ma (Goldblatt et al. 2008) or (46.5-)36.7(-27.6) Ma (Joyce et al. 2018).
6. Nivenioideae Goldblatt
Plant with woody stem; monocot secondary thickening +; vessel elements in roots with scalariform perforation plates only; leaves with non-vascular fibrous strands; unit of rhipidium with 1-2 flowers; flowers long-lived, sessile; T long-tubular, (short-tubular, T long-linear - Klattia); endothecial cells with basal anastomosis of U-shaped thickenings; (pollen grains with encircling sulcus); stigmas simple, not or somewhat expanded; ovules 2/carpel (-6), endostomal, outer integument 2-3 cells across; 1 shield-shaped seed per loculus [seed tangentially flattened]; exotesta transparent, mesotesta 0-1 cell across; n = 16.
3/14. Only in the S.W. Cape region, South Africa
Age. Crown-group Nivenioideae are estimated to be (33.5-)23.3(-13.6) Ma (Joyce et al. 2018).
6. Crocoideae G. T. Burnett
Plant with corms; vessel elements in root with simple perforation plates; (mesophyll cells laterally elongated); (leaf vernation plicate), when flat with pseudomidrib (not Pillansia), sheath closed; inflorescence spicate; rhipidium binate, with a single flower, pedicel 0; (flowers short-lived), variously monosymmetric (polysymmetric); endothecial cells with spiral thickenings; pollen exine tectate, perforate-scabrate, aperture with one or a pair of longitudinal bands forming operculum, (zona-/in-/spiraperturate/polyrugate); late-acting self incompatibility [Crocus]; (septal nectaries 0); (ovules campylotropous), nucellar columella +, hypostase prominent, postament +; chalazal endosperm haustorium +; n = 3-17, etc., (karyotype bimodal).
28/1020: Gladiolus (260), Geissorhiza (97), Romulea (90), Crocus (100 or 235), Hesperantha (80), Babiana (55), Watsonia (50), Ixia (50), Lapeirousia (27). Overwhelmingly southern African, to Europe, Madagascar and Central Asia.
Age. Crown-group Crocoideae are only ca 24 Ma (Goldblatt et al. 2008) or (34.6-)26.7(-19.7) Ma (Joyce et al. 2018).
Synonymy: Crocaceae Vest, Galaxiaceae Rafinesque, Gladiolaceae Rafinesque, Ixiaceae Horaninow
Evolution: Divergence & Distribution. It has been suggested that Iridaceae were originally from Antarctica-Australia. The family then achieved its current distribution by a mixture of long-distance dispersal across a proto-Indian Ocean and migration via west Antarctica to Africa and the New World where the family is currently very diverse (e.g. Sanmartín & Ronquist 2004; Goldblatt et al. 2008).
Davies et al. (2005) noted that in Iridaceae diversification was greater in areas like southern Africa than in the northern hemisphere, and that there were clades with a disproportionately large number of species in e.g. southern Africa. The Cape area is notably diverse from a global point of view (Kreft & Jetz 2007), and Iridaceae are one of the major geophytic groups of the Cape flora (Procheŝ et al. 2006, also Linder 2003) with more than 650 species there in at least two major clades, or 1,050 species in southern Africa as a whole (S. D. Johnson 2010). The great majority of these species have specialized pollination mechanisms and are typically pollinated by only a single pollinator species (Johnson & Steiner 2003; Goldblatt & Manning 2006). Davies et al. (2004c) see this diversification as the result of the interaction of local features such as the ecological and climatic heterogeneity of the area, and this affects reproductive isolation. Valente at al. (2012) suggested that pollinator shifts had helped drive speciation in southern African Gladiolus, although other factors were also involved. For the radiation of the Cape genus Moraea, both cytologically and florally diverse, see Goldblatt et al. (2002, 2005: pollination; Galley et al. 2007: also diversification on the Drakensbergs); radiation in this and other iridaceous Cape genera may have begun in the fynbos in the Miocene some 25 Ma, divergence in the succulent Karoo being more recent (Verboom et al. 2009). Diversification of two geophytic Cape genera, Babiana, with ca 92 species nearly all from the Greater Cape floristic region, and Moraea, with over 150 species in the Cape region, may in part be connected with soil type preferences changing during speciation; here diversification began a mere 17-15 Ma in the mid-Pliocene (Schnitzler et al. 2011); diversification rates in the Cape region and outside are largely similar (Silvestro et al. 2011).
Manning and Goldblatt (1991) suggest apomorphies for Nivenioideae.
Pollination Biology & Seed Dispersal. Iridaceae show considerable floral diversification, ranging from the open flowers of Sisyrinchium to the meranthia of Iris et al. (for which, see Guo 2015b) and the tubular flowers of Gladiolus et al. (e.g. Bernhardt & Goldblatt 2006; Goldblatt & Manning 2006 and references; Rodrigues & Sytsma 2006; C. A. Wilson 2006). In Iris and its relatives the flower will appear to the pollinator as if were really three monosymmetric flowers (e.g. Westerkamp & Claßen-Bockhoff 2007). The tepaloid style overarches the stamen opposite it and the landing platform for the pollinator is the member of the outer perianth whorl that lies directly underneath the style/stamen complex. However, in Cypella the three landing platforms for the pollinating bees are members of the inner perianth whorl. Here the pollen deposited on the backs of the bees comes from half anthers of adjacent stamens and is deposited on the receptive surfaces of two adjacent half-stigmas (Vogel 1974).
The flowers of Gladiolus (Crocoideae) are obliquely monosymmetric, although this is hardly apparent in the open flower due to changes in orientation as the flower and inflorescence grow. Tepal patterning, where it occurs, is usually on an adaxial lateral tepal of the outer whorl and adjacent members of the inner whorl and is clearly on the adaxial side of the flower, but it may be on an adaxial lateral and the abaxial member of the outer whorl and a tepal of the inner whorl between them (Eichler 1875; Choob 2001). Although other Crocoideae may have the same oblique monosymmetry, Lapeirousia and Ixia, for example, may have monosymmetric flowers with normal monocot orientation. Flowers in Diplarrena (Iridoideae) are similar, but they have only two stamens and one staminode. Interesting infraspecific variation occurs. In some flowers of Crocosmia X crocosmiiflora the odd member of the outer whorl was adaxial while in others it was abaxial; the patterning of the tepals, etc., varied accordingly (pers. obs.). All told, well over half the family has monosymmetric flowers of one sort or another, and the evolution of monosymmetry in the family will repay further study (see also Davies et al. 2004b).
Much work on pollination in Iridaceae has been carried out by Peter Goldblatt and John Manning, species from the sub-Saharan region of Africa, especially from South Africa, being the focus of their research. Nearly all species have morphologically specialized flowers and are pollinated by non-specialist (if sometimes highly specialized) pollinators (Goldblatt & Manning 2006, 2008 for general accounts; S. D. Johnson 2010). Floral homoplasy is very extensive in Iridoideae-Tigridieae (Rodrigues & Sytsma 2006), -Trimezieae (Lovo et al. 2012), and -Irideae (in Iris itself - C. A. Wilson 2006). Many different kinds of pollinators are involved, and even in quite small southern African genera of Iridaceae a variety of different pollinators are involved, e.g., dung flies, long-tongued bees, wasps and beetles all pollinate Ferraria, which has only 17 species (Goldblatt et al. 2009, see also 2000a: Ixia, 2000b: Sparaxis). Babiana (Crocoideae) is pollinated by birds, scarab beetles, bees, moths, etc. (Bernhardt & Goldblatt 2006; esp. Goldblatt & Manning 2007), while scarabeid monkey beetles pollinate the flowers of three Cape genera of Iridaceae that have distinctive dark markings at the bases of the tepals (van Kleunen et al. 2007). Valente at al. (2012) examined pollination in southern African Gladiolus, recording numerous gains and losses of five of the seven pollination syndromes (the other two were decidedly uncommon), with long-tounged bee pollination being acquired at least four or twelve times (depending on the method used), but lost twice as frequently or more (see also Goldblatt et al. 1998b; Goldblatt & Manning 2002), there were 17 pollinator shifts in the 23 species of Lapeirousia studied (Forest et al. 2014: more important in speciation that changes in substrate specificity). For a discussion on the evolution of the complex appendages, etc., on the sepals of bearded irises and their ilk, see Guo (2015a, b).
At least 34 species of southwest African Iridaceae are known to be pollinated by three species of (extremely) long-tongued dipteran nemestrinid flies, and all told slightly over 10% (117 species) of the 1,050 species of Iridaceae in southern Africa have such pollinators. The long-tubed monosymmetric flowers pollinated by these flies have evolved several times, both here and in unrelated groups (Manning & Goldblatt 1996, 1997; Goldblatt & Manning 2000, 2006), and Karolyi et al. (2013) discuss how the flies take in the nectar. Only 64 species of Iridaceae in the same region are bird pollinated, but over 550 species are pollinated by long-tongued Apidae (Goldblatt & Manning 2006).
There are a number of oil flowers in Iridaceae, including the South American Cypella (see above), ca 35 species of Sisyrinchium, also from South America, and some other New World Iridoideae like Tigridia (Renner & Schaefer 2010; Possobom & Machado 2017a and references). In nearly all cases, the elaiophores are made up of mats of unicellular trichomes (Tölke et al. 2019), and these appear to have evolved twice in Sisyrinchium alone (Chauveau et al. 2011). Indeed, these trichomes vary both in morphology and position in flowers of New World Iridaceae (Silvério et al. 2012); evolution of floral rewards in these taxa has a complex pattern of gains, changes and losses (Chauveau et al. 2012).
Some species of Nivenia are heterostylous (Sánchez et al. 2010; Cohen 2019), a rather uncommon condition in the monocots.
Bacterial/Fungal Associations. Details of the nature of the presumably mycoheterotrophic association of Geosiris are unclear (Imhof et al. 2013).
Vegetative Variation. Some Iridaceae are more or less woody and have monocot-type secondary thickening (see above); the vessel elements in the roots of such plants often have predominantly scalariform perforation plates (Cheadle 1964: inc. Klattia).
Foliar variation is considerable. Leaves may be terete and unifacial or apparently ordinary and heterobifacial (e.g. some Iris), very commonly they are ensiform and isobifacial, as in Gladiolus and most Iris, others like those of Crocus can be strangely ribbed, but in transverse section they all seem to be variations of a basic isobifacial leaf theme (e.g. Ross 1892, 1893; Arber 1925; Rudall 1991). Some of this variation is ontogenetic: in Iris, for example, seedlings may have terete leaf blades, while those of adults are ensiform and isobifacial (Rudall & Buzgo 2002). Geissorhiza alone has ligulate leaves. There are water-catching leaves with very distinctive morphologies found especially in taxa from Namaqualand, South Africa (Vogel & Müller-Doblies 2011). For leaf morphogenesis, including the development of plications, see Rudall (1990b). There are also terete and laterally flattened isobifacial leaves in Juncaceae.
Genes & Genomes. A genome duplication event, the SIANα event, date at ca 81.3 Ma, characterizes the Iridaceae (Landis et al. 2018). Moraes et al. (2015) looked at the evolution of chromosome numbers (very variable) in Iridoideae, and also gave some 2C values. Although polyploid species had the highest 2C values, both polyploids and diploids had medium-sized to small genomes. For cytological evolution in Crocus, n = 3<, see Harpke et al. (2013); multiple hybridizations, dysploidy events, and evolution of B chromosomes are all involved.
For the biparental transmission of plastids in crosses of Louisiana irises, see Cruzan et al. (1993). Joyce et al. (2018) discuss the evolution of the chloroplast genome in the mycoheterotrophic Geosiris.
Economic Importance. Mykhailenko et al. (2019) provide an entry to the literature on saffron, the stigmas of Crocus sativus; at around $600-$1000/kg (retail is higher), it is a very expensive spice...
Chemistry, Morphology, etc.. Several distinctive metabolites occur here, e.g. plumbagin in Aristea and Homeria and bufadienolides (cardiac glycosides) in Moraea (Iridoideae) (Harborne & Williams 2001). Iris contains a greater diversity of isoflavonoids than any other group outside Fabaceae (Reynaud et al. 2005); for xanthones, especially in Iris, see C. A. Williams et al. (1997b).
Goldblatt (1990) interpreted the paired "bracts" below the single flowers of Isophysis as representing a reduced rhipidium, a monochasial cymose inflorescence - a rhipidium may then be another synapomorphy for the whole family. Aristea is palynologically very variable, some members even having disulcate pollen (see Goldblatt & Le Thomas 1997; le Thomas et al. 2001). Crocus has spiraperturate pollen or variants of this, and there is quite substantial infraspecific variation in pollen morphology (Candan & Özhatay 2013 and references: Crocus chrysanthus, also variation in chromosome number). The occurrence of septal nectaries needs to be checked. In Sisyrinchium and its relatives the style branches alternate with the stamens; elsewhere the two are usually on the same radius. For a discussion of the caruncles/arils of Iris, see C. A. Wilson (2006). Galil (1968 and references) noted that in at least some species of Iris the plumuule descended down the hollowed primary root, the corm thus developing below the surface of the ground.
Additional general information is taken from Goldblatt et al. (1998a), Goldblatt (2001), and Goldblatt and Manning (1998: Gladiolus, 2008: generic accounts); see also Rodionenko (1987), Mathew (1989) and Crespo et al. (2015), Iris s.l., Rübsamen-Westenfeld et al. (1994), Merckx et al. (2013a: general), Imhof et al. (2013: roots, mycorrhizae)\ and Gray and Low (2017), all Geosiris, and Kerndorff et al. (2016a), Crocus. For meta carboxy aromatic amino acids, see Larsen et al. 1981) and for the phytochemistry of Crocus, see Mykhailenko et al. (2019), Rudall et al. (1986) and Rudall (1984: secondary thickening, 1995a) discuss anatomy, Goldblatt et al. (1984) crystals; see also Cocucci and Vogel (2001) and Rudall et al. (2003a), both nectary evolution, Manning and Goldblatt (1990) endothecial thickenings, Dönmez and Isik (2008: pollen), Venkateswarlu et al. (1980), C. A. Wilson (2001), Steyn (1973a, b) and Dorofeeva and Zhurbenko (2020: Iris), all embryology, Kerndorff et al. (2016b: seed morphology in Crocus), Wand and Hasenstein (2016) seed coat stomata, and Tillich (2003a) seedlings - very variable.
Phylogeny. Iridaceae are monophyletic in nearly all studies (but c.f. Chase et al. 1995a). Initial results suggested that the monotypic Isophysidoideae were sister to the rest of the family, Crocoideae and Iridoideae appeared to be monophyletic, but the status of Aristeoideae was unclear. Reeves et al. (2001a, b: four genes) found that Patersonia, Geosiris, and Aristea were successively sister to a large clade making up [Aristeoideae + Crocoideae]; support was mostly moderate (see also Teixeira de Souza-Chies et al. 1997). If these relationships were confirmed, either the circumscription of Crocoideae would have to be considerably extended, or three more subfamilies would be needed. Goldblatt et al. (2008: five plastid genes) took this latter option; they found strong support for the pectinations basal to Crocoideae s. str., albeit using successive weighting, which tends to leave one a little uneasy; the topology above was also recovered by Joyce et al. (2018) in a generic-level reanalysis of Goldblatt et al.'s data. See Rudall (1994c) for a morphological phylogeny.
Within Iridoideae the morphologically very distinctive Australian Diplarrhena may be sister to the rest (Reeves et al. 2001a, b; Rudall et al. 2003a). The five tribes in Iridioideae are quite well supported and have well-resolved relationships: [Diplarreneae [Irideae [Sisyrinchieae [Trimezieae + Tigridieae]]]] (Goldblatt & Manning 2008; also Golblatt et al. 2004, 2006). Irideae. For a phylogeny of Iris, see Tillie et al. (2001) and C. A. Wilson (2004); there is phylogenetic resolution of the major groups in the genus (Wilson 2011), although some of the characters used to distinguish groups in the past, such as sepal crests (ridges or more elaborate structures down the midrib of the outer perianth whorl) have turned out to be homoplasious (Guo & Wilson 2014). Wilson et al. (2016) looked at relationships within the royal irises (sect. Oncocyclus) and Wilson (2017) at relationships within the bearded irises (subgenus Iris). Sisyrincheae. Karst and Wilson (2012) obtained a fair degree of resolution in relationships within Sisyrinchium, although species limits there are in a considerable state of disarray (see also Chauveau et al. 2011); Inácio et al. (2017) provide a detailed phylogeny of the genus, and found that S. chilense and S. elegantulum were the result of wide crosses. For diversification in the American Tigridieae, see Rodrigues and Sytsma (2006). Relationships within Trimezieae are being clarified (Lovo et al. 2012, 2018).
The five tribes of Crocoideae were mostly only moderately supported and their relationships poorly resolved in a study by Goldblatt and Manning (2008; also Goldblatt et al. 2004). Tritoniopsis, with a tubular cotyledonary sheath and tubular cataphyll, may be sister to the rest of the subfamily, but support is at best moderate (Goldblatt et al. 2006; Golblatt & Manning 2008). For a phylogeny of Crocus see Petersen et al. (2008, c.f. in part Frello et al. 2004), and especially Harpke et al. (2013) and Kerndorff et al. (2016a, b). For relationships within Gladiolus, see Valente et al. (2011, 2012); although there was some resolution towards the base of the tree, many species, especially those from southern Africa, could not be distinguished.
Classification. I follow the classification suggested by Goldblatt et al. (2008; see also Goldblatt et al. 1998; Goldblatt & Manning 2015: Lapeirousia and relatives); the subfamilies are for the most part well characterised. Lovo et al. (2018) circumscribe genera in Trimezieae. Inácio et al. (2017) provide an infrageneric classification for Sisyrinchium). See C. A. Wilson (2011, also e.g. 2017) for an infrageneric classification of Iris, which Crespo et al. (2015) have split into twenty five genera (and see another classification in Rodionenko 2009)...
[Xeronemataceae [Asphodelaceae [Amaryllidaceae + Asparagaceae]]]: ovary superior; mitochondrial rpl2 gene lost.
Age. Estimates of the age of this node are around (84-)74, 67(-57) Ma (Bell et al. 2010), ca 100 Ma (Janssen & Bremer 2004), and (78-)69(-60) or ca 55.8 Ma (S. Chen et al. 2013).
Evolution: Divergence & Distribution. The loss of the mitochondrial rpl2 gene occurs either at this node or the next up the tree (see Adams et al. 2002b).
Phylogeny. This is a strongly supported group in Fay et al. (2000) and Soltis et al. (2007a); see also Janssen and Bremer (2004).
XERONEMATACEAE M. W. Chase, Rudall & Fay - Back to Asparagales
Plant rhizomatous; leaves two-ranked, ventralized isobifacial [oriented edge on to the stem]; inflorescence branched, with inflorescence bracts, densely spicate; flowers large; stamens long-exserted, anthers centrifixed; pollen boat-shaped; style solid; ca 8 ovules/carpel, ?embryology; seeds bluntly papillate; n = 17, 18, x = 9 (?8), nuclear genome [1 C] (0.277-)3.803(-52.157) pg.
1 [list]/2. New Zealand (Poor Knights Island) and New Caledonia.
Chemistry, Morphology, etc.. The family is little known, although there is some information in Chase et al. (2000c); the style is scored as if it is hollow in Rudall (2003a).
Previous Relationships. Xeronemataceae were provisionally included in Asphodelaceae by Takhtajan (1997) and in Hemerocallidaceae by Clifford et al. (1998).
[Asphodelaceae [Amaryllidaceae + Asparagaceae]]: (pedicels articulated); septal nectaries infralocular; ovules with parietal tissue 2-3 cells across.
Age. The age of this node is some (72-)64, 58(-49) Ma (Bell et al. 2010), ca 93 Ma (Janssen & Bremer 2004), 75.9 or 81.4 Ma (Tank et al. 2015: Table S2), 61-54 Ma (Wikström et al. 2001), (72-)63(-55) or ca 43.6 Ma (S. Chen et al. 2013), 67.6 Ma (Magallón et al. 2015) or (60.4-)54.2(-50.4) Ma by D.-F. Xie et al. (2020).
Evolution: Divergence & Distribution. For the optimisation of characters like "septal nectaries infralocular" and "ovary superior", see the beginning of this page. The optimisation of successive microsporogenesis on the tree is also uncertain (Chase et al. 2000a); for instance, microsporogenesis varies within Asphodelaceae.
Chemistry, Morphology. Gatin (1920: broad sampling across Liliaceae s.l.) found that taxa that have tepals with single vascular traces are common in this clade, although some have three or more traces; she also studied many other details of pedicel vasculature. Schnarf and Wunderlich (1939) provide embryological details and El-Hamidi (1952) some for the gynoecium from scattered taxa in "Asphodeloideae"; the latter found substantial similarity between all the taxa he examined except Aphyllanthes (Asparagaceae-Aphyllanthoideae). For chromosome sizes of a number of taxa in the group, see Vijayavalli and Mathew (1990 - as Liliaceae).
Phylogeny. This clade was early found to have strong support (Fay et al. 2000; Chase et al. 2000b).
ASPHODELACEAE Jussieu, nom. cons. - Back to Asparagales
Anthraquinones +, fructan sugars accumulated; roots (vessel elements with simple perforation plates), styloids +; leaf sheath closed; inflorescence scapose; pedicels articulated; (A not adnate to T); late-acting self incompatibility [all?]; outer integument ³3 cells across, hypostase +; x = 8 (?7), nuclear genome [1 C] (0.263-)3.209(-39.203) pg; cotyledon not photosynthetic.
41/900-1,060. Esp. Old World, not Arctic, western South America.
Age. This crown group is dated to ca 90 Ma (Janssen & Bremer 2004). Bell et al. (2010), on the other hand, estimate an age of (66-)52, 47(-36) Ma, S. Chen et al. (2013) a variety of ages - (66-)56(-48), ca 47, or ca 39 Ma, while (85-)74, 68(-60) Ma is the age in Crisp et al. (2014), 52.3 Ma in Magallón et al. (2015) and (73/3-)71.3(-69.4) Ma in McLay and Bayly (2016).
1. Asphodeloideae Burnett
Often rosette-forming leaf succulents, geophytic (rhizomatous) herbs to pachycaul trees, (climbers); tetrahydroanthracenones + [e.g. chrysophanol], anthrone-C-glycosides [in leaves], 11-methyl-8-hydroxyanthraquinone [in root]; (velamen +); (monocot secondary thickening +); sieve tube plastids with peripheral fibres in addition to the central protein crystal - Aloë group); foliar vascular bundles often inverted, parenchymatous cells in the inner bundle sheath adjacent to the phloem [aloin cells], (cells sclerenchymatous); leaves spiral or two-ranked, margins often with spines, (bases not sheathing); inflorescence racemose, branched or not, (spicate), (not scapose); (pedicels not articulated), monosymmetry +, ± weak [Haworthia et al.]; flowers tubular, T ± free (connate - Kniphofia, etc.), (with a single trace); (anthers centrifixed); microsporogenesis simultaneous; (pollen mixed with raphides); stigma dry (wet); ovules 1-many/carpel, hemitropous, (± straight - Asphodelus clade), outer integument 3-4 cells across, parietal tissue 1 (2) cells across, hypostase +; (embryo sac tetrasporic, three chalazal megaspores fuse, divide twice [Fritillaria-type] - Eremurus); (fruit a berry); seed ± angled/(winged), aril +, funicular (thin/0); endosperm thick-walled, hemicellulosic[?], (perisperm +, slight), embryo long; n = (6 - Kniphofia) 7, chromosomes 1.5-20 µm long, karyotype usu. bimodal; 3'-rps12 intron lost; (coleoptile +).
19 [list]/785-940: Aloë (400-560), Kniphofia (70), Bulbine (60), Trachyandra (50), Eremurus (45), Haworthia (42). Africa, esp. South Africa; also the Mediterranean to Central Asia, Australia, New Zealand. Map: see Reynolds (1966), Frankenberg and Klaus (1980) and Seberg (2007). Photo: Collection, Inflorescence, Flowers.]
Age. Crown-group Asphodeloideae are estimated to be (46-)34(-25) or ca 22.5 Ma (S. Chen et al. 2013) or (75-)69-58(-51) Ma (Crisp et al. 2014: see discussion after Xanthorrhoeoideae, the two models not differing here).
Synonymy: Aloaceae Batsch
[Xanthorrhoeoideae + Hemerocallidoideae]: raphides 0.
Age. The age of this node is (63-)52.5(-45) or ca 46.4 Ma in S. Chen et al. (2013) or rather older, (71.2-)67.1(-62.5) Ma, in McLay and Bayly (2016). Note that the age of Xanthorrhoea stem in Crisp et al. (2014) is based on the topology [Hemerocallidoideae [Xanthorrhoeoideae + Asphodeloideae]].
The 47.8-38 Ma fossil Dianellophyllum eocenicum from Central Australia has been placed on the stem node of Hemerocallidoideae (Iles et al. 2015).
2. Xanthorrhoeoideae M. W. Chase, Reveal & M. F. Fay
Stem thick, woody, erect (not); plant resiniferous; monocot secondary thickening +; layer of sclerenchyma below epidermis in leaves, stomata paracytic; leaves spiral, unifacial, persistent, leaf base not sheathing, internodes short; inflorescence long-scapose, densely spike-like, branches cymose, congested; flowers sessile, not articulated; flowers ± tubular, T = 3 dry + 3 subpetal-like, free; stamens long exserted, spreading; microsporogenesis successive [tetrads tetragonal]; pollen extended sulcate; stigma ± punctate, ?wet; ovules several/carpel, outer integument ca 3 cells across, apex of nucellus pointed, hypostase?; inner cuticle of tegmen +; seeds flattened; endosperm quite thick-walled, development?, little hemicellulose, embryo transverse to long axis of seed; n = 11, (karyotype bimodal); hypocotyl short.
1[list]/30. Australia (map: from Australia's Virtual Herbarium, i.2015). [Photo - Habitat, - Habit, Inflorescence.]
Age. Crown-group Xanthorrhoeoideae are estimated to be a mere (3.8-)1.7(-0.3) Ma (S. Chen et al. 2013) or (59-)35-24(-13) Ma (Crisp et al. 2014), although the latter also obtained some very young ages, most in the range of (13-)6.4, 3.3(-1.8) Ma, one somewhat older. Crisp et al. (2014) preferred the older (first) estimates, which came from using a random local clocks model, over the younger ages, which came from an uncorrelated lognormal relaxed clock model; the latter, they thought, could not handle the substitution rate changes.
Synonymy: Xanthorrhoeaceae Dumortier, nom. cons.
3. Hemerocallidoideae Lindley
Habit various; flavonols, naphthoquinones, saponins +; roots often swollen; (vessels in the stem); mucilage cells 0; stomata anomocytic, cuticular wax rodlets parallel; leaves (spirally) two-ranked (equitant), vernation conduplicate to flat-conduplicate or plicate, (semi-ensiform, isobifacial), (margin serrulate); (inflorescence not scapose); (bracteoles lateral), flowers (monosymmetric); (median tepal of outer whorl adaxial - Hemerocallis), T tube short (1/2 connate - Hemerocallis/0); filaments often ornamented/swollen, anthers (centrifixed), dehiscing by pores/coiled after anthesis - Dianella and relatives); microsporogenesis simultaneous (successive), pollen trichotomosulcate (tetrachotomosulcate, monosulcate), usu. <30µm across, pollenkitt +; stigma dry (wet), (3-parted - Pasithea); ovules 1-many/carpel, outer integument 4-7 cells across, inner integument 2-4 cells across, parietal tissue none, nucellar cap ca 2 cells across (0), podium well developed, hypostase 0; antipodal cells large, persistent; fruit also a berry (nut); seeds ovoid, (flattened - Phormium), (with strophiole/aril - Johnsonia et al.); endosperm hemicellulosic, usu. helobial, embryo not central [Geitonoplesium], also short; n = 4 [Agrostocrinum], 8, 9, 11, 12, chromosomes 0.8-17.33 µm long; (cotyledon not photosynthetic - Dianella), epicotyl long or not, (hypocotyl 0; collar +), primary root well developed, branched or not.
20[list]/89: Dianella (40 or more). Papuasia to New Zealand and the Pacific, esp. Australia (e.g. all 8 genera of Johnsonieae s. str.), also Europe to Asia, Malesia, India, Madagascar, Africa; two genera and two species in South America (map: from Fl. Austral., Wurdack & Dorr 2009; Muscat et al. 2019: figs 2, 3 - Dianella). [Photo - Habit, Flower, Flower].
Age. Crown-group Hemerocallidoideae are (53-)45(-36) or ca 39 Ma (S. Chen et al. 2013) or (63.6-)58(-52.4) Ma (McLay & Bayly 2016).
A fossil, Dianellophyllum eocenicum, from the Middle Eocene has been collected from Lake Eyre, in Central Australia, and is quite similar to Dianella (Conran et al. 2003).
Synonymy: Dianellaceae Salisbury, Eccremidaceae Doweld, Geitonoplesiaceae Conran, Hemerocallidaceae R. Brown, Johnsoniaceae J. T. Lotsy, Phormiaceae J. Agardh
Evolution: Divergence & Distribution. For additional divergence dates within Hemerocallidoideae, see McLay and Bayly (2016). The subfamily is Australian with the exception of the Eurasian Simethis and Hemerocallis, and one species of Dianella in Zimbabwe (see Muscat et al. 2019: Figs 2, 3 for the distribution of the genus) which makes things biogeographically interesting (McLay & Bayly 2016).
Asphodelaceae-Asphodeloideae are very diverse (ca 340 species) in southern Africa (Johnson 2010) where Aloe started diversifying ca 16 Ma (Grace et al. 2015), moving north in Africa and with a major accumulation of species (>130, representing several dispersal events) on Madagascar (Dee et al. 2018). Eccremis and Pasithea represent independent migrations of the phormioid clade (Hemerocallidoideae) to South America (Wurdack & Door 2009), while Bulbinella (Asphodeloideae) grows in South Africa and New Zealand.
Some diversification in Xanthorrhoea may be associated with the aridification of the Nullarbor Plain some 14-13 Ma that separated eastern and western clades (Crisp & Cook 2007).
Chomicki et al. (2017b) look at the evolution of plant architecture in the Aloe area - most species have Tomlinson's and Corner's mpdels, some Leeuwenberg's. Both Hemerocallidoideae and Xanthorrhoeoideae have ovaries that can be interpreted as being secondarily superior and that have infra-locular septal nectaries (Rudall 2002, 2003a).
Ecology & Physiology. For an ecological account of Xanthorrhoea, see Lamont et al. (2004); the genus has quite deep roots. The plant grows in flammable savanna/shrubby vegetation and itself burns easily, but the apical meristem is unharmed and there is often post-fire flowering (fast-flammable: Pausas et al. 2017)
Pollination Biology & Seed Dispersal. Many species of the large genus Aloë (Asphodeloideae), perhaps some 85 species in southern Africa alone, but into Arabia, too, are pollinated by birds (Rebelo 1987; McCoy 2019), short-billed birds other than typical nectar-eaters visiting some species with dark-coloured and bitter-tasting nectar that are not deterred by its taste (Johnson et al. 2006). There is also insect pollination, perhaps especially among the short-tubed species (Symes et al. 2009; Hargreaves et al. 2008, 2012; McCoy 2019), as in other groups of Asphodelaceae, and also bat pollination (Dee et al. 2018). Buzz pollination probably predominates in Hemerocallidoideae, and the small pollen (but c.f. Arnocrinum and Hemerocallis), although not the presence of pollenkitt, is consistent with this (Furness et al. 2014).
A number of Hemerocallidoideae have myrmecochorous seeds (Lengyel et al. 2010). Interestingly, the baccate fruits of the Lomatophyllum group of Aloë have winged seeds (Dee et al. 2018).
Vegetative Variation. Most members of the Hemerocallidoideae have leaves that are more or less isobifacial immediately above the sheath, but higher up they become dorsiventrally flattened and more "normal" in appearance; Pasithea, sister to the rest of the clade, lacks this isobifacial zone (Wurdack & Dorr 2009), so it is unlikely to be an apomorphy for the subfamily. Geitonoplesium has resupinate leaves.
Members of Asphodeloideae have more or less succulent leaves, and species of Aloë and Haworthia in particular are commonly rosette plants with massively fleshy leaves (e.g. Melo-de-Pinna 2016); these can be borne in spirals or be distinctively two-ranked; seedlings/young plants may have two-ranked and adults spiral leaves (e.g. McCoy 2019). The vascular bundles in the leaf of Aloe may form a circle and there are globules in the outer bundle sheath (also in Kniphofia); the central cells of the leaf are gelatinous. As with Aizoaceae from southern Africa, there is great variation in the micromorphology of their epidermis (Cutler 1982); the two grow in similar extreme habitats. For the remarkable water-catching leaves in taxa growing in foggy deserts in Namaqualand, South Africa, see Vogel and Müller-Doblies (2011).
Clifford (1998) noted that seedlings of Xanthorrhoea had two-ranked leaves, those of the adult are spirally arranged.
Aloin cells are reported from Dianella (Hemerocallidoideae: see Rudall 2003a); on the other hand, Kniphofia lacks them, having a well developed sclerenchymatous cap in their place (as have some other Asphodelaceae, even some Alooideae). It is unclear if aloin cells are secretory (Beaumont et al. 1985: survey and chemistry).
Genes & Genomes. A genome duplication of crown-group Hemerocallidoideae, the PHTEα event, has been dated to 37.8 Ma (Landis et al. 2018).
Some species of Bulbine have a bimodal karyotype of n = 7, 4 long and 3 short (Spies & Hardy 1983), rather like the karyotype of Aloeae (4L + 3S: Chase et al. 2000a; Devey et al. 2006; Pires et al. 2006); they probably evolved independently, and the plants also have similar medicinal properties...
Chemistry, Morphology, etc.. The old Alooideae (= Asphodeloideae, part) are chemically very distinctive (Klopper et al. 2010 for a summary). Aloin, an anthraquinone glycoside, is a laxative commonly found in Aloë. 1-methyl-8-hydroxyanthraquinones, e.g. chrysophanol, are commonly found in the roots and anthrone-C-glycosides in the leaves (e.g. Manning et al. 2014). In other Asphodeloideae, Bulbine, Trachyandra, and Kniphofia all have knipholone, an anthraquinone derivative (van Wyck et al. 2005), but it appears not to have been reported from the Asphodelus clade. There is chelidonic acid in Johnsonia (Hemerocallidoideae) (Ramstad 1953).
The apical meristem of the stem in Xanthorrhoea media is massive - 580-1283 µm across (Staff 1968, q.v. for details of stem growth). The old Alooideae are reported to have tetracytic stomata (e.g. Cutler 1972), although this is questioned by G. Smith and van Wyk (1992).
The inflorescences of Xanthorrhoea are described as being terminal (Clifford 1998); they are sometimes axillary in Asphodeloideae. Within Hemerocallidoideae the flowers of Hemerocallis seems to have a lateral bracteole, as do those of Dianella; both may have "inverted" flowers (e.g. Eichler 1875; Ehrhardt 1992), although in Hemerocallis, at least, this seems to be variable. Hemerocallis flowers with the median outer tepal adaxial are common, but the seal of the Daylily Society shows a flower with the normal monocot orientation. The number of vascular bundles supplying the tepals in members of this subfamily varies from (1-)3-9(-25) (Clifford et al. 1998a) and the stamens are often rather elaborate. In at least some species of Aloë the larger stamens are opposite the inner whorl of tepals.
Microsporogenesis in Hemerocallis was described as being successive and the endosperm as being nuclear by Di Fulvio and Cave (1965, but c.f. Cave 1948, 1955) and Yan et al. (2017: intermediate microsporogenesis). Hemerocallis also has isoflavones, monosulcate pollen and a wet stigma, but it lacks a nucellar cap and septal nectaries. There are conflicting reports about embryo sac development (Yan et al. 2017 and references). In pollen morphology Hemerocallis was considered to be derived by Chase et al. (1996); with Simethis, which has trichotomosulcate pollen, it is sister to the rest of Hemerocallidoideae (see also McPherson et al. 2004; Wurdack & Dorr 2009; Furness et al. 2014: microsporogenesis in Simethis?), so monosulcate pollen in Hemerocallidoideae may be a reversal. Since Chamaescilla also has monosulcate pollen (McLay & Bayly 2016), the story becomes more complicated.
Ovule orientation at the basal node in the family is unclear (c.f. Steyn & Smith 1998). Kniphofia has a bistomal micropyle and a nucellar endothelium (Takhtajan 1985). Daru et al. (2013) noted that seedlings of Aloë and Gasteria have two-ranked leaves, whatever the leaf arrangement in the adults.
For general information, see G. Smith and Van Wyk (1998), Clifford and Conran (1998: Johnsoniaceae), Clifford et al. (1998a: Hemerocallidaceae), Grace and Rønsted (2017: Asphodeloideae), also Reynolds (1966, 2004), Carter et al. (2011), Frandsen (2017), esp. Aloë, well illustrated, and Smith and Figueirwedo (2020: Asphodeloideae), also Riley and Majumdar (1979: biosystematics), Van Wyk et al. (1996, 2005), Viljoen et al. (1998: Aloe flavonoids), Grace et al. (2010) and Kite et al. (2000: anthroquinones), all chemotaxonomy, G. Smith et al. (1992: anatomy), Ely and Luque Arias (2006: anatomy of Eccremis), Kosenko (1994: pollen of Phormium), Furness et al. (2014: pollen of Hemerocallidoideae), Shamrov (2014a: gynoecium of Hemerocallis), Eunus (1952), Raju (1957), Berg (1962), di Fulvio and Cave (1965), Cave (1975) and Zuo and Ma (2014), all embryology, Steyn and Smith (1998: ovule morphology, 2001) and Thadeo et al. (2015: fruit anatomy).
For Xanthorrhoea, some information is taken from Chanda and Ghosh (1976: pollen), Rudall (1994b: embryology), Rudall and Chase (1996: phylogeny) and Bedford et al. (1986) and Clifford (1998), both general.
Phylogeny. There is strong support for Asphodelaceae s.l. (in much recent literature the name used has been Xanthorrhoeaceae s.l.) in Fay et al. (2000), Wurdack and Dorr (2009), etc.. However, relationships within the clade were initially unclear. There is slight support for a [Xanthorrhoeoideae + Asphodeloideae] clade in the three-gene tree of Chase et al. (2000a; see also Fay et al. 2000; Crisp et al. 2014: chloroplast genes); some analyses in Chase et al. (2000a) also suggested an [Asphodeloideae + Hemerocallidoideae] clade. Hemerocallidoideae, and perhaps also Asphodeloideae, were paraphyletic in a rpb2 analysis of Crisp et al. (2014: ?rooting). However, Devey et al. (2006) found support for a [Xanthorrhoeoideae + Hemerocallidoideae] clade (see also Pires et al. 2006; Graham et al. 2006; Wurdack & Dorr 2009: good-moderate support; Seberg et al. 2012; Steele et al. 2012: strong support; Hertweck et al. 2015; S. Chen et al. 2013). Rudall (2003a) suggested that there were close morphological relationships between Hemerocallidaceae and Asphodelaceae - and between Xanthorrhoeaceae and Iridaceae...
Within Asphodeloideae, Aloë and its immediate relatives (= Alooideae s. str.: Klopper et al. 2010 for a summary) seem distinct and form a monophyletic group. However, more ordinary-looking Bulbine (for a phylogeny, see Devey et al. 2006) is sister to this clade, and then come other Asphodeloideae, including Kniphofia et al. and Eremurus et al., which together form a clade (Naderi Safar et al. 2014); an [Asphodelus + Asphodeline] clade (n = 14) is sister to the rest of the subfamily, and with good support (see Devey et al. 2006, also references below; McLay and Bayly 2016). Ramdhani et al. (2009) discussed the phylogeny of Kniphofia. For relationships around Aloë, which remained poorly understood and little resolved for some time and still present problems, see Treutlein et al. (2003a, b), Grace et al. (2015) and Dee et al. (2018). Ramdhani et al. (2011) looked at relationships around Haworthia, and Daru et al. (2013) and in particular Manning et al. (2014) have clarified relationships there, although support for some of the basal branches could be improved, and species of both Aloë and Haworthia are still scattered through the tree.
Rudall and Chase (1996) and Crisp and Cook (2007) have looked at the phyogeny of Xanthorrhoea.
There are two well supported clades within Hemerocallidoideae, the phormioid and johnsonioid (= hemerocalloid + johnsonioid) clades (e.g. Wurdack & Dorr 2009; also Seberg et al. 2012; Crisp et al. 2014). The loss of the 3'-rps12 intron characterises the johnsonioid clade (= [Johnsonieae [Hemerocallis + Simethis]]), see McPherson et al. (2004) and Chase et al. (2000b). Chamaescilla (ex Asparagaceae-Lomandroideae) has quite recently been found to be sister to the [Hemerocallis + Simethis] clade (McLay & Bayly 2016). Pasithea, from South America, is sister to all other phormioids (Wurdack & Dorr 2009; Seberg et al. 2012; Crisp et al. 2014). The other New World genus, Eccremis, previously of uncertain relationships (e.g. Clifford et al. 1998a) because of interpretations of morphology, is sister to Dianella (Wurdack & Dorr 2009), of the phormioid clade; similar relationships were also recovered by McLay and Bayly (2016) and Muscat et al. (2019), the latter group carrying out an extensive study of relationships in Dianella.
Classification. A.P.G. II (2003) suggested as an option the inclusion of Asphodelaceae, Xanthorrhoeaceae and Hemerocallidaceae in Xanthorrhoeaceae s.l., and this circumscription was adopted by A.P.G. III (2009), but because of nomenclatural issues the name of this clade has been changed to Asphodelaceae (A.P.G. IV 2016), otherwise, see Chase et al. (2009b). The recognition of an Alooideae (= Asphodeloideae-Aloeae) would make Asphodeloideae paraphyletic and necessitate the recognition of several other weakly characterized subfamilies.
G. Smith and Steyn (2004) discuss the taxonomy of Alooideae; generic limits around Aloë are decidedly unsatisfactory. Grace et al. (2013) and in particular Manning et al. (2014) have revised the classification of the whole group, recognising 11 genera (see also Rowley 2015), but it is clear that there is still work to do, the species of genera like Lomatophyllum being scattered around Aloë and sectional limits in the latter are problematic (Dee et al. 2018). Several intergeneric hybrids have been described from Asphodeloideae (Smith & Figueiredo 2020 and references), but their existence depends on generic limits...
Species limits are particularly difficult in Aloë, in Kniphofia (Ramdhani et al. 2009), and in Haworthia (Bayer 2009; Ramdhani et al. 2011: ?hybridization), all Asphodeloideae. Species estimates in Dianella (Hemerocallidoideae) range from 25-350+ (Carr 2007); the phylogeny in Muscat et al. (2019) suggests that the number will be well above 40.
Previous Relationships. Three genera that used to be placed in Asphodelaceae s. str., i.e. in Asphodelaceae-Asphodeloideae, are now in Hemerocallidoideae (Simethis), Asparagaceae-Asparagoideae (Hemiphylacus), and Asparagaceae-Agavoideae (Paradisea, Anthericaceae s. str.) respectively, while Chamaescilla, which used to be in Asparagaceae-Lomandroideae, has moved to Asphodelaceae-Hemerocallidoideae - the evidence is largely molecular (Chase et al. 2000b; McLay & Bayly 2016).
Thanks. I thank Syd Ramdhani and Matt Ogburn for useful discussions.
[Amaryllidaceae + Asparagaceae]: microsporogenesis successive [possible place]; endosperm development?
Age. This node is ca 91 Ma (Janssen & Bremer 2004), ca 71.5 Ma (Tank et al. 2015: Table S2), 58-51 Ma (Wikström et al. 2001), (69-)60, 54(-45) Ma (Bell et al. 2010), (67-)41(-50) or ca 41.6/40.6 Ma (S. Chen et al. 2013), about 62.5 Ma (Magallón et al. 2015) or (50.6-)49.4(-48.2) Ma (D.-F. Xie et al. 2020).
Evolution: Ecology & Physiology. Grime and Mowforth (1982) early noted links between large genomes in the taxa they examined (focus on the British flora), the geophytic habit, and fast growth by cell expansion of large cells (link to large genomes) under cooler conditions in the spring - geophytes are quite common in this clade.
Genes & Genomes. For chromosome size in Liliaceae s.l. and relatives, i.e. including some taxa in this area, see Vijayavalli and Mathew (1990).
Chemistry, Morphology, etc.. Steroidal saponins are particularly common in taxa in this part of the tree; records in older literature can be found under Liliaceae.
Microsporogenesis is uniform here. In other Asparagales with successive microsporogenesis, details of wall formation (centrifugal cell plates) is similar to those members of this clade that have been studied, however, plate formation may also be centripetal when microsporogensis is simultaneous (Nadot et al. 2006). Johri (1966) provides some infomation about stylar morphology; the style can become solid in more than one way.
Phylogeny. This is a strongly supported clade (e.g. Chase et al. 1995a; Fay et al. 2000; Chase et al. 2000b; Graham et al. 2005), however, inclusion of Aphyllanthes in analyses has tended to decrease support for the clades within it (Graham et al. 2006; Givnish et al. 2018a). Kim et al. (2011: seven genes, three compartments) found that Amaryllidaceae grouped with Asparagoideae, Lomandroideae and Nolinoideae; other members of this clade formed a separate group.
AMARYLLIDACEAE J. Saint-Hilaire, nom. cons. - Back to Asparagales
Fructan sugars accumulated; root vessel elements with scalariform perforation plates; leaves two-ranked; inflorescence scapose, umbellate, cymose, inflorescence bracts 2 or more, scarious, floral bracts small; pedicels not articulated; flowers large [>1.5 cm long and across]; (T free); (A connate basally); style long, stigma dry; parietal tissue none; endosperm nuclear or helobial; x = 8 (?9), nuclear genome [1 C] (0.674-)8.187(-99.495) pg; hypocotyl 0.
73/1605. Worldwide - three subfamilies below.
Age. Estimates of the age of crown-group Amaryllidaceae are ca 87 Ma (Janssen & Bremer 2004), (62-)51(-42) or ca 33.7 Ma (S. Chen et al. 2013), (51-)44.7(-42) Ma (Han et al. 2019) or(77.2-)67.9(-58.5) ma (Costa et al. 2020).
Evolution: Ecology & Physiology. Ma et al. (2018) noted that Amaryllidaceae, despite their herbaceous habit, had rather thick first-order roots.
Bacterial/Fungal Associations. Fungi on Allium and other Allioideae are rather different from those on Amaryllidoideae (e.g. Savile 1962).
Genes & Genomes. For cytological evolution, see Costa et al. (2020). Very large genomes with a C value of some 350 picograms or more are found in some Amaryllidaceae-Allioideae and -Amaryllidoideae - and also in Asparagaceae-Scilloideae (Leitch et al. 2005).
Chemistry, Morphology, etc.. Distinctive, mannose-binding lectins (the specificity is absolute) are found in Allioideae and Amaryllidoideae (van Damme et al. 1991: known from Agapanthus?; see also Peumans & van Damme 1995; Vandenborre et al. 2011). For tapetal cells, see Wunderlich (1954), for inflorescence structure, see Weberling (1989).
Phylogeny. This is a very strongly supported clade (e.g. Fay et al. 2000, but c.f. McPherson et al. 2004; Thomas et al. 2005), and it has some characters! Meerow et al. (1999), Fay et al. (2000: strong support), Givnish et al. (2006), Pires et al. (2006) and Seberg et al. (2012: support weak) suggest a set of relationships [Agapanthaceae [Alliaceae + Amaryllidaceae]]. However, Meerow et al. (2000a) found Agapanthaceae to be sister to Amaryllidaceae, albeit with weak support, and these relationships were also recovered by Costa et al. (2020) and dated to (68.4-)62.7(-55.8) Ma.
Classification. Combining the three families Agapanthaceae, Alliaceae and Amaryllidaceae into Alliaceae s.l. was an option in A.P.G. II (2003), an option that was exercised in A.P.G. III (2009), although under the name of Amaryllidaceae. The infrafamial classification follows that in Chase et al. (2009b).
1. Agapanthoideae Endlicher
Plant rhizomatous; steroidal saponins +; velamen +; laticifers +?; leaf vernation flat; inflorescence bracts connate along one side, other bracts?; flowers weakly monosymmetric; T ± connate basally; anther middle layer of wall from outer secondary parietal cells; ovules apotropous; seeds flat, winged; endosperm with starch/hemicellulose, embryo short; n = (14) 15 (16), chromosomes 4-9 µm long; seedling as in Allioideae?
1 [list]/9. South Africa (map: from Leighton 1965). [Photo - Habit, Flower.]
Chemistry, Morphology, etc.. Information is taken from Kubitzki (1998b: general) and D. Zhang et al. (2010: reports of occasional embryos with two cotyledons, 2011: embryogeny).
Synonymy: Agapanthaceae F. Voigt
[Allioideae + Amaryllidoideae]: plants geophytes, bulbous, bulbs tunicate, with contractile roots; lectins binding mannose; (corona +); (embryo sac bisporic, eight nucleate - Allium type).
Age. This node is estimated to be (62-)50, 46(-35) Ma by Bell et al. (2010) and (56.5-)47(-38), ca 30.3 Ma by S. Chen et al. (2013) or (47.6-)41.9(-34.5) ma (D.-X. Xie et al. 2020). Janssen and Bremer (2004) estimate that the stem-group age of this clade is ca 91 Ma.
2. Allioideae Herbert
Flavonoids, cysteine-derived sulphur compounds +; root vessel elements often with simple perforation plates; raphides often 0, styloids +; laticifers +; leaves (spiral), sheath closed, long; bracts enclosing inflorescence 2, ± connate; flowers medium sized [<1 cm long, <1.5 cm across]; T ± connate; A connate or adnate to free; style solid, (stigma wet); ovules 2-many/carpel, collateral/2-seriate, campylotropous (anatropous), (micropyle bistomal), parietal tissue 0, nucellar cap +/0, obturator +; embryo sac bisporic, eight nucleate [Allium type]; seeds angular, exotestal, other layers of testa collapsed or not; (endosperm pitted), suspensot 2-tiered; chromosomes 2-20 µm long; (cotyledon not photosynthetic).
13[list, to tribes]/795. Mainly South America, but Allium esp. N. Temperate Eurasia - three groups below. [Photo - Collection] [Photo - Inflorescence, Flower, Flower.]
Age. Crown-group Allioideae are estimated to be ca 87 Ma (Janssen & Bremer (2004), (44.5-)37(-28) or ca 30.3 Ma (S. Chen et al. 2013), (44.5-)41.4(-35.8) Ma (Han et al. 2019) or (67.5-)63.2(-53.7) ma (Costa et al. 2020).
2A. Allieae Dumortier
Bulbs with membranous scales [?level]; starch 0, spiranostanol steroidal saponins +; (plant ± rhizomatous); root exodermis multilayered, cortex not differentiated (yes), stele narrow, unmedullated; leaves ± unifacial, (shortly ligulate); bracts enclosing inflorescence 2-5; T basally connate/free, with one trace; A basally connate, adnate to C, filaments often winged, at least basally, tapetal cells uninucleate; (G semi-inferior), style ± gynobasic, solid, (paired projections from the ovary); ovules epi-/apotropous, outer integument 4-6 cells across, inner integument ca 3 cells across, (suprachalazal zone massive - A. fistulosum); (seed with caruncle); endosperm cellular, embryo long, curved; n = (7) 8 (9-11), chromosomes 9.0-19.3 µm long, TTAGGGn [human-type] telomeric repeats lost; (germination cryptocotylar).
1/ca 660. North temperate, often seasonally dry, especially in the Mediterranean to Central Asia and west North America, scattered in Africa (map: from Hultén 1962; de Wilde-Duyfjes 1976; Hanelt 1990; Hanelt et al. 1992; Fl. N. Am. 26: 2002, not native in Iceland).
Age. Crown-group Allieae are (45.8-)34.3(-24.3) Ma (Q.-Q. Li et al. 2016), (39.9-)33.5(-27.3) Ma (Han et al. 2019), (58.1-)52.2(44.4) Ma (Costa et al. 2020) and (34.8-)22.2(-15.2) Ma (D.-F. Xie et al. 2020), while the estimate in Hauenschild et al. (2017) is a mere (14.4-)12.8(-11.2) Ma.
Paleoallium has been described by Pigg et al. (2018) from deposits ca 49.4 Ma in Washington, U.S.A.; it certainly does look like Allium!
Synonymy: Alliaceae Borkhausen, nom. cons., Cepaceae Salisbury, Milulaceae Traub
[Tulbaghieae + Gilliesieae]]: bulbs with starch; corona +; endosperm helobial; embryo short; x = 6.
Age. This node is ca 37-32 Ma (Sassone & Giussani 2018) or (65.1-)54.1(-37.1) Ma (Costa et al. 2020).
2B. Tulbaghieae Meisner
Plant rhizomatous; leaf sheath short; flowers bracteate; T rather strongly connate, corona massive, 3-lobed, lobes connate or not [opposite inner T]; A sessile, adnate to T tube and/or corona; style solid by enlargement of epidermal cells of cavity; seeds ± flattened; n = 6, chromosomes 11.5-14.7 µm long.
1/20. Southern Africa (map: from Vosa 1975; Trop. Afr. Fl. Pl. Ecol. Distr. 7. 2012).
Synonymy: Tulbaghiaceae Salisbury
2C. Gilliesieae Baker
Stigma ± 3-lobed; x = 6/?5, karyotype bimodal, nuclear genome [1 Cx] 23.1-23.9 pg.
11/77-115. Southeast U. S. A. to Central America, western South America (inc. southwest Brazil) to Chile. (Map: from Fl. North America 26. 2002.)
Age. The age of this node is ca 31.8 Ma (Sassone & Giussani 2018), (61.2-)ca 45(-32.2) Ma (Costa et al. 2020) or ca 50.0 Ma (Escobar et al. 2020).
(Rhizomes +); steroidal saponins +, (sulphur compounds ?0 [plant not smelling]); inflorescence (1-)many-flowered; A (variously basally connate and adnate), (staminodes 3, 6); G (shortly stipitate), stigma (capitate), papillate; (embryo sac monosporic, eight nucleate [Polygonum type] - Nothoscordum); seeds black; x = 5, n = (4-)5(-7, etc.), nuclear genome [1Cx] 9.07-30.46[-60.6(-79.3)?] pg.
6/65-100<: Nothoscordum (25-80). South U.S.A., Mexico to Chile, most South America, but not in the NE.
Age. Crown-group Leucocoryninae are (35-)27.5(-25) Ma (Sassone & Giussani 2018) or ca 37.1 Ma (Escobar et al. 2020).
2Cb. Gilliesiinae Bentham & J. D. Hookerr
Flowers ± monosymmetric/not; T (3 - Schickendantziella)/(3 + 3 reduced); (corona 0); A (2/3), ± free, (connate), (staminodes 3); septal nectaries ?0; ?embryo sac; n = 6, 7, 10, chromosomes 5.5-14.9 μm long, nuclear genome [1C] 18.4-31.1 pg.
5/17. Peru to Chile.
Age. Crown-group Gilliesiinae are (29-)18(-7) Ma (Sassone & Giussani 2018) or ca 25.6 Ma (Escobar et al. 2020).
Synonymy: Gilliesiaceae Lindley
Evolution: Divergence & Distribution. For additional dates in Leucocoryninae, see Sassone and Giussani (2018) and in Allium, see Han et al. (2019) and D.-F. Xie et al. (2020).
Costa et al. (2020) obtained rather older dates for/within Allioideae than other workers, and focussing on the Southern Hemisphere, they interpreted the biogeography of the group partly in terms of vicariant events, for example, Allium rafted north on India.
Nguyen et al. (2008) found that Old and New Word species of Allium are mostly in two separate clades. Basal to the clade containing all North American members of Allium (in subgenus Amerallium) are European taxa, and there are two other main clades that are made up of Eurasian and Central-West Asian taxa respectively (see also e.g. Friesen et al. 2006; Han et al. 2019). Diversity within North America Allium is centred in the west, especially in California, and a number of species there are serpentine endemics (Nguyen et al. 2008). Q.-Q. Li et al. (2016) looked at biogeographical relationships within subgenus Anguinum, which is made up of a clade restricted to eastern Asia and another that is found throughout the northern hemisphere. Han et al. (2019) suggested that polyploidy was involved in the diversification of the genus, along with shifts to habitats with different soils.
Pollination Biology & Seed Dispersal. Gilliesia has very strongly monosymmetric flowers with only two stamens; the flowers may mimic insects (Rudall et al. 2002). For septal nectaries and where nectar ends up in the flower, see Vogel (1998b).
Vegetative Variation. The apparently bifacial leaves of at least some species of Allium have inverted vascular bundles along the adaxial surface and vascular bundles with normal orientation along the abaxial surface (Mathew 1996). In a comprehensive study, Mashayekhi and Columbus (2014) looked at the leaf anatomy of 67 species of Allium, finding i.a. that species with terete, unifacial leaves might have a ring of bundles or a single series of normally oriented bundles, and species with flattened leaves sometimes had two series of normally-oriented bundles.
Genes & Genomes. Messeri (1931) and Vosa (1975, 2000: Tulbaghia) discuss aspects of cytology. Within Leucocoryninae there has been hybridization, polyploidy, and also Robertsonian translocations (i.e., karyotype change by chromosome fusion or breakage at the centromere), and the extremes of genome size are represented by Ipheion (low) and Leucocoryne (high) - altogether genome evolution has been very active in this clade (Sassone et al. 2017). Allium has lost its TTAGGGn telomere minisatellite terminal sequence repeats, and although some species do have this repeat, it is not telomeric (Sýkorová et al. 2006a).
There has been a major movement of several ribosomal protein genes and the succinate dehydrogenase gene from the mitochondrion in Allium (Adams et al. 2002b; Adams & Palmer 2003). The genome in is in three circles, and the gene involved in cytoplasmic male sterility, at least in the S-type cytoplasm of “Momiji-3” (Allium cepa), is orf 725 (Tsujimura et al. 20118).
Economic Importance. Caterpillars of the leek moth, Acrolepiopsis assectella (Yponomeutoidea-Glyphipterigidae), are major pests of leeks and onions (Sohn et al. 2013).
Chemistry, Morphology, etc.. Allium is well known for producing steroidal saponins, perhaps some 290 or so kinds (Sobolewska et al. 2016). The root anatomy of Allium (Fritsch 1992) is very distinctive compared with that of other Asparagales (Kauff et al. 2000).
The flowers of Allium are shown with the median member of the outer whorl in the adaxial position (Spichiger et al. 2004). Schickendantziella (Gilliesiinae) has only three tepals; they are caudate. Coronal structures in Gilliesiinae vary in number and are often more or less linear; it has been suggested that they may be staminodial in some species (ref.?), but this is unlikely since the number of stamens + linear processes usually = >6, and taxa with more than six stamens are uncommon in this part of the tree. Do all Allioideae have apotropous ovules? Vosa (2000) implies that Tulbaghia has an Allium-type embryo sac.
Some information is taken from Rahn (1998) and Sassone et al. (2014: Leucocoryneae), both general, and Sundar Rao (1940), Berg (1996) and Berg and Maze (1966), all embryology. For Allium, see Rabinowitch and Currah (2002: more horti-/agricultural), R. M. Fritsch and Friesen (2002 - and many other papers in same book), all general, R. M. Fritsch and Keusgen (2006: cysteine sulphoxide distribution), Choi et al. (2011: floral development, esp. epidermis), Vinogradova (2018: endosperm development), Kruse (1988) and Celep et al. (2012), both s.e.m. seeds, Messeri (1931: embryology), and Druselmann (1992: much info. on germination).
Phylogeny. Fay and Chase (1996) discuss relationships within the subfamily; the topology is [Allieae [Tulbaghieae + Gilliesiae]], although the support for the clades is rather weak while relationships in Escobar et al. (2020) are [[Allieae + Tulbaghieae] Gilliesiae].
Within Leucocoryneae/Leucocoryninae, Fay et al. (2006b) found that part of Ipheion was embedded in Nothoscordum, sister to the rest of the group. For relationships around Leucocoryne, see Souza et al. (2015, 2016), Sassone et al. (2017), Sassone and Giussani (2018) and Escobar et al. (2020), [Leucocoryne + Latace] are sister to the remainder of the group. Gilliesieae. Escobar et al. (2020) found that Gilliesia and Miersia were paraphyletiv. Allieae. Nguyen et al. (2008) provide a phylogeny for Allium and find that there are three main clades (see above, also Friesen et al. 2006; Hirschegger et al. 2010: section Allium; Huang et al. 2014; Han et al. 2019: comprehensive analysis); the relationships of members of the small subgenera Nectaroscordum and Microscordum have been unclear (Nguyen et al. 2008; Mashayekhi & Columbus 2014). For relationships in subgenus Amerallium, which includes nearly all North American species, see Choi et al. (2012), Q.-Q. Li et al. (2012) and Mashayekhi and Columbus (2014: most sections not monophyletic), and for those within the small subgenus Anguinum, see Li et al. (2016). In the large subgenus Melanocrommyum, many species of which are to be found in the Qinghai-Tibet region (111 species of the genus grow there), there seems to be extended incomplete lineage sorting, and morphological sections are not supported by molecular data (Gurushidze et al. 2008, esp. 2010; see also Hauenschild et al. 2017: subgenera not monophyletic, Gurushidze not mentioned).
Classification. See Fay and Chase (1996: as Alliaceae). Friesen et al. (2006) provide a subgeneric and sectional classification of Allium which has since been elaborated (see above); Gregory et al. (1998) list names included in it. For the contents of Leucocoryninae, see Sassone et al. (2014).
3. Amaryllidoideae Burnett - Back to Asparagales
Norbelladine alkaloids, non-protein amino acids, chelidonic acid +, saponins 0; roots contractile, (velamen +, 2-4-layered), medulla often 0; sclerenchymatous ring in scape, bundles in rings; foliar (vascular bundles inverted), basal bundles in arc; (lacunae formed by breakdown of parenchyma); leaves (spiral), vernation flat or revolute to involute, (base sheathing); bracts equitant[?]; flowers large; T with median member of outer whorl adaxial, ± free; anther middle layer of wall from outer secondary parietal cells; (tapetal cells uninucleate); G inferior, stigma capitate to deeply trifid, (wet); (ovule with outer integument ³3 cells across), (inner integument to 4 cells across), (nucellar cap to 3 cells across); endosperm starchy or with hemicellulose, (thin-walled), embryo poorly differentiated, small; x = 11, chromosomes (1.5-)3-28 µm long; cotyledon bifacial, (not photosynthetic), primary root well developed, contractile.
Ca 75 [list: to tribes]/900 - fourteen tribes below. Tropical (temperate), esp. South America and Africa, also Mediterranean (map: from Alan Meerow and O. Seberg, pers. comm.; Snijman 1984; Fl. N. Am. 26: 2002; de Castro et al. 2012). [Photo - Flower, Fruit.]
Age. Crown-group Amaryllidoideae are (39-)28.5(-19) or ca 15.9 Ma (S. Chen et al. 2013).
3A. Amaryllideae Dumortier
(Growth monopodial - Crinum); stomata paracytic, subsidiary cells with oblique divisions; extensible [helically-thickened] fibres in leaf; leaves follow the flowers, (perennial - many Crininae), spiral or 2-ranked; filament corona + [of webbing joining filaments basally, or small appendages developed from filaments], or 0 [Crinineae]; tectal cells binucleat; pollen bisulcate, exine gemmate, with scattered spinules, intectate-columellate; style solid apically [Crinum], (laterally displaced); ovules unitegmic (ategmic; parietal tissue 0 - Crinum); embryo sac bisporic, 8-celled [Allium type], (antipodal cells persistent); seeds water-rich, non-dormant, phytomelan 0, testa multiplicative, to 25 cells thick, chlorophyllous, with stomata/± collapsed/0, cork layer in endosperm [Crinum]; endosperm chlorophyllous, usu. with a corky layer, starchy, embryo chlorophyllous; (n = 10, 12, 15), chromosomes 5.3-20.5 µm long.
11/146: Crinum (65), Strumaria (23). SubSaharan, especially South Africa, Crinum Pantropical.
Synonymy: Crinaceae Vest, Strumariaceae Salisbury
Calostemmateae, etc.: bundle sheath cells parenchymatous.
[Calostemmateae [Cyrtantheae + Haemantheae]]: ?
3B. Calostemmateae D. & U. Müller-Doblies
Ovules 2-3/carpel; embryo germinates precociously producing a bulbil; fruit dry, indehiscent; phytomelan 0; n = 10, chromosomes 3.3-8 µm long.
2/4. Australia, Malesia.
[Cyrtantheae + Haemantheae]: 1-layered rhizodermis +, velamen 0; scape lacking sclerenchymatous ring, subepidermal collenchyma +; fruit indehiscent.
3C. Cyrtantheae Traub
Leaves ; scape hollow; flowers poly- to strongly monosymmetric; (A with basal appendages connate, forming 12-lobed corona); late-acting self incompatibility; seeds flat, winged, horizontally stacked; n = (7) 8 (11).
1/56 (Cyrtanthus). Africa, mainly the South.
Synonymy: Cyrtanthaceae Salisbury
3D. Haemantheae Hutchinson
(Plant rhizomatous - Clivia, Scadoxus); (alkaloids 0 - Gethyllis [= G.]); leaves spirally arranged, blade spirally twisted/narrowly linear/with dense long white hairs/etc.; scape 2-angled; inflorescence bracts several, equitant, (T-like); (flowers single - G., etc.), (densely aggregated - Haemanthus); (A 6-fasciculate, 6-8 A/fascicle - G.); (filament corona +); late-acting self incompatibility [all?]; fruit baccate; seeds angled/embedded in fleshy pulp/etc.; phytomelan 0 (+ - Cryptostephanus); n = 6, 8, 9, 11, 12; chromosomes 3.0-24 µm long.
6/80: Gethyllis (39, inc. Apodolirion), Haemanthus (22). Tropical Africa, mostly in the South.
Synonymy: Gethyllidaceae Rafinesque, Haemanthaceae Salisbury
[[Lycorideae [Galantheae, Pancratieae, Narcisseae]] [[Griffinieae + Hippeastreae] [Eustephieae [Eucharideae [Hymenocallideae, + Clinantheae]]]]]: ?
[Lycorideae [Galantheae, Pancratieae, Narcisseae]] / Eurasian Clade: seeds subglobose, turgid.
3E. Lycorideae D. Müller-Doblies & U. Müller-Doblies
Spathe 2-valved; stigma ± capitate/3-lobed; 2-many ovules/carpel; (seeds irregularly discoid - Ungernia); n = (8, 10) 11.
3/27: Lycoris (20). Temperate to subtropical East Asia, to Iran.
[Galantheae, Pancratieae, Narcisseae]: ?
3F. Galantheae Parlatore
(Roots not medullated); (inflorescence bracts connate along one side); (anthers dehiscing by pores); parietal tissue +; embryo sac bisporic, 8-celled [Allium type; elaiosome + (0); n = 7-9, 11, 12, nuclear genome size [1Cx] -82.2 pg [Galanthus lagodechianus].
8/31: Galanthus (17). Europe to N. Africa, the Crimea and the Caucasus.
Synonymy: Galanthaceae G. Meyer, Leucojaceae Borkhausen
3G. Pancratieae Dumortier
Leaves spiral; filament corona + [filaments joined by toothed tube]; style solid apically; n = 11, chromosomes 8.7-22 µm long.
1/20. Mediterranean, southern Asia, to sub-Saharan Africa.
Synonymy: Pancratiaceae Horaninow
3H. Narcisseae Lamarck & de Candolle
(Roots not medullated); inflorescence bracts basally connate; (tepalline corona + [tubular - Narcissus]); (heterostyly + [Narcissus]); late-acting self incompatibility [Narcissus]; parietal tissue to 2 cells across, ?nucellar cap +; embryo sac bisporic, 8-celled [Endymion-type]; elaiosome + (0); n = (7) 11 (13), etc.; nuclear genome (14.3-)14.5-67.7(69.7) ... (93.6-)96.3(-99) pg.
2/58: Narcissus (?50). Europe to W. Asia and N. Africa.
Age. Crown-group Narcisseae are ca 23.6 Ma (Santos-Gally et al. 2012) or ca 13.8 Ma (Marques et al. 2017).
Synonymy: Narcissaceae Jussieu
[[Griffinieae + Hippeastreae] [Hippeastreae [Eustephieae [Eucharideae [Hymenocallideae + Clinantheae]]]] / Andean + Extra-Andean/American Clade: 1-layered rhizodermis +, velamen 0; scape lacking sclerenchymatous ring, subepidermal collenchyma +; bracts obvolute; (seeds flat, horizontally stacked), phytomelan common.
[Griffinieae + Hippeastreae]: ?
3I. Griffinieae Ravenna
Velamen + [Worsleya]; flowers blue; seeds whitish, globose, turgid [Griffinia]; n = 10, 21.
3J. Hippeastreae Sweet
(Leaves pseudopetiolate); inflorescence bracts 2, ± connate or not; flowers (very strongly) monosymmetric/polysymmetric, odd member of the outer whorl adaxial/abaxial; T tube short to long, (tepalline corona +, short, morphology various); A declinate (not), of varying lengths; style solid [Zephyranthes], stigma capitate or 3-lobed; seeds flattened, winged or D-shaped, (elaiosome +); n = 6-9, 11, chromosomes 3-16.7 µm long.
6/200: Zephyranthes (175), Hippeastrum (105). S.E./S.W. U.S.A., the Caribbean, and Central and South America.
Synonymy: Brunsvigiaceae Horaninow, Oporanthaceae Salisbury, Zephyranthaceae Salisbury
[Eustephieae [Eucharideae [Hymenocallideae + Clinantheae]]] / Andean Tetraploid Clade: palisade leaf mesophyll absent; flowers polysymmetric (slightly monosymmetric); seeds flattened, winged; x = 23 [tetraploid], nrITS1 with two indels.
Age. Meerow et al. (2020) suggest that this clade may be ca 30.9 Ma, although at the same time they wonder if this is somewhat too old.
3K. Eustephieae Hutchinson
Scape ± flattened/angled; A of two lengths; (corona +, free from filaments); (n = 21, etc.).
3/15: C. Andes (Peru, Bolivia, Argentina).
Age.The age of crown-group Eustephieae is estimated to be around 24.1 Ma (Meerow et al. 2020).
[Eucharideae [Hymenocallideae + Clinantheae]]]: nrITS2 with indel.
Age. This node is ca 28.7 Ma (Meerow et al. 2020).
3L. Eucharideae Hutchinson [inc. Stenomesseae]
Leaves petiolate, elliptic; (flowers monosymmetric); filament corona [staminal cup] + (0); pollen (in tetrads); (globose nectary glands at base of A - Eucrosia); seeds (globose, turgid, coat lustrous; endosperm oily); chromosomes 2.3-10.7 µm long; plastome ndhF 0, other ndh genes pseudogenized.
6/90: Stenomesson (35), Eucharis (17). Central America, the Andes S. to Bolivia.
Age. This clade is aroun 12 Ma (Meerow et al. 2020).
[Hymenocallideae + Clinantheae]]]: ?
Age. The age of this clade is approximately 28.1 Ma (Meerow et al. 2020).
3M. Hymenocallideae Small
Leves (pseudopetiolate); scape ± flattened/angled; filament corona +; pollen (>100 μm long), ends of grains narrowed, with different sculpture [± auriculate]; ovules (many/carpel); testa thick, spongy, chlorophyllous, vascularized, phytomelan 0 (+ - Leptochiton); embryo starchy, (polyembryony +); (n = 12, 17, 19, 20, 22, 23), chromosomes 4-11.8 µm long.
3/65: Hymenocallis (50). S.E. U.S.A., the Antilles, Southern Mexico to Bolivia.
Age. Crown-group Hymenocallideae are around 26.1 Ma (Meerow et al. 2020).
3N. Clinantheae Meerow
(Epiphytic/epilithic); (velamen + - Pamianthe); seeds flattened, obliquely winged.
3/. Columbia to Bolivia and Peru.
Age. The age of this cladeis ca 26.9 Ma (Meerow et al. 2020).
Evolution: Divergence & Distribution. Meerow (2010) discussed diversification in American Amaryllidaceae in terms of the interplay of canalization and genome doubling, emphasizing the floral and vegetative diversity encompassed by the Andean tetraploid-derived clade. Santos-Gally et al. (2012) discussed the biogeography of the Mediterranean-centred Narcissus, the two main clades in the genus diversifying within the last 10 Ma as dry grassy vegetation became established in the western Mediterranean (Marques et al. 2017). Meerow et al. (2020) discussed the biogeography of the Andean Tetraploid Clade, which has reached the southeastern United States (Hymenocallis) in some detail. About a third of the subfamily, 240-280 species, grow in southern Africa, and around 85% of these are found nowhere else (Johnson 2010; Duncan et al. 2016, 2020).
Petiolate leaves have evolved at least six times in the family (?ref).
Ecology & Physiology. Amaryllidoideae are an important component of the distinctive Cape geophytic flora (Procheŝ et al. 2006) having about 100 species endemic there. For water-catching leaves with very distinctive morphologies that are found especially in taxa from Namaqualand, South Africa, see Vogel and Müller-Doblies (2011).
Pollination Biology & Seed Dispersal. Monosymmetry is thought to be ancestral in the subfamily (Meerow & Snijman 1998; Meerow 2010). It is certainly very labile, reversals and parallelisms being common, and it is perhaps under simple genetic control (Meerow et al. 1999). Some kind of corona is common, but its morphological nature varies (see below). The flowers are protandrous. A number of species of Amaryllis are di- or tristylous (Graham & Barrett 2004; Santos-Gally et al. 2013 and references).
Bird pollination is quite important in Amaryllidoideae. A. Meerow (pers. comm. ii.2014) estimated that around 100-150 species in South America (genera like Brunswigia, Hippeastrum, Stenomesson) may be pollinated by humming birds, while in southern Africa ca 13 species of Cyrtanthus alone are pollinated by sunbirds (Snijman & Meerow 2010). Several other kinds of pollinators service Cyrtanthus, including hawk moths, which may pollinate ca 22 species of Amaryllidoideae from southern Africa (Manning & Snijman 2002). Pollination of some red-flowered taxa there is by largish butterflies, which get pollen on their wings from the brush-type flowers/inflorescences and transmit it to other flowers; this type of pollinatioin may be derived from bird pollination (Butler & Johnson 2020 and references).
Almost three hundred species in the subfamily have myrmecochorous seeds (Lengyel et al. 2010). Wind dispersal of the seed is common in Amaryllideae, and the rigid, radiating pedicels of taxa like Boophone allow the infructescences to bowl along in the wind. The testa is commonly massive, green and photosynthetic, and with anomocytic stomata in Amaryllidinae, while in Crinum the endosperm is green and photosynthetic. Seeds of some species lack a testa but have a corky outer endosperm, and they can float and remain viable in sea water for up to two years; seeds of other species lack the corky layer and sink fast - in fact they can germinate without very much in the way of water at all (Snijman & Linder 1996; Bjorå et al. 2006). In Boophone and Cybistetes the seeds germinate while still in the fruit, while in Calostemmateae the bulbil, actually a precociously-germinated embryo, is the dispersal unit. Gethyllis (Haemantheae) has a single-flowered inflorscence and the flowers have a subterranean ovary. Here the fruit is baccate and grows just above the surface of the ground and is sometimes sweetly scented when ripe; the seeds are reported to be embedded in fleshy pulp (Duncan et al. 2016, 2020), perhaps dispersal by small mammals?
Vegetative Variation. Robertson (1906) described the inflorescences of Galanthus and Leucojum as being lateral, the stem being monopodial; stalked bulblets were produced. Gethyllis (Haemantheae) in particular shows remarkable foliar variation, and some species have collars (?= a sheathing leaf base) surrounding the leaves, which are narrow to broad, spirally twisted or not, and with variable indumentum (Duncan et al. 2016, 2020). Vogel and Müller-Doblies (2011) describe water-catching leaves with very distinctive morphologies that are found especially in Namaqualand, South Africa.
Genes & Genomes. A genome duplication for crown-group Amaryllidaceae, the AGAFα event, occurred an estimated 50.1 Ma, and a duplication for Amaryllidoideae, the NAVIβ event, ca 41.2 Ma (Landis et al. 2018). x = 11 may be the basal chromosome number for the family (Meerow et al. 2006). There has been a reduction in the GC content of the genome, perhaps associated with the large genome sizes found here (Smarda et al. 2014). For genome size in Narcissus and its correlation with taxonomy, see Zonneveld (2008; see also Marques et al. 2017). Poggio et al. (2014) found that the bimodal karyotype of Hippeastrum remained largely constant in morphology despite changes in chromosome numbers and genome size/genome, and overall genome size changed relatively less. For the extensive karyotypic evolution in Gilliesieae, where there has been much Robertsonian change (i.e. chromosome fusion or breakage at the centromere) and polyploidy, see Pellicer et al. (2017).
García et al. (2014, 2017) discuss the likelihood that there was extensive and ancient hybridization in Hippeastreae-Hippeastrinae, ca six events being likely, and with incomplete lineage sorting in the stem clades, although not in -Traubiinae. Marques et al. (2017) emphasized that there had been much hybridization, including between members of different subgenera, in Narcissus.
Chemistry, Morphology, etc.. Norbelladine alkaloids, unique to Amaryllidoideae, are tyrosine derivatives. There are over 500 different structures, of which 79 or more are found in Narcissus alone, placed in 118 different classe (Martin 1987; Bastida & Viladomat 2002: other references in the same volume; Rønsted et al. 2008b, 2012; papers in South African J. Bot. 136. 2021). These alkaloids cause i.a. acetylcholinesterase inhibition, etc., in Haemantheae (Bay-Smidt et al. 2011) and Calostemmateae (Jensen et al. 2011); see also Nair et al. (2016). For their synthesis, see Kilgore et al. (2016).
Because of the leaf fibres in Amaryllideae, the coverings of the bulbs produce highly-extensible cotton-like fibres when torn. There are often crystals of calcium oxalate in the foliar epidermis. Weiglin (2001) documented quite a variety of epicuticular wax morphologies in Gethyllis.
The flowers of Galanthus are shown with the median member of the outer whorl in the adaxial position (Spichiger et al. 2004), see also the similar position in Hippeastrum and several other monosymmetric Amaryllidoideae. Some species of Phaedranassa have slit-monosymmetric flowers, with all the stamens, etc., leaving the flower via an abaxial slit in the perianth tube; I do not know details of the symmetry there. Flowers of some species of Crinum are monosymmetric. In Galanthus in particular the inner whorl of tepals is very different from the outer whorl, although both are petal-like.
The morphologies of the corona of e.g. Hymenocallis, paired evascularized outgrowths of the filaments, and that of Narcissus, vascularized and tubular (see also Scotland 2013) and not immediately associated with the stamens, are quite different (e.g. Arber 1937); the corona may also be a tube, sometimes toothed (Pancratium), on which the stamens are born. Haemanthus has tepals with a single trace. In Strumaria and Carpolyza the bases of the filaments are adnate to the style, while in Strumaria and Tedingia the base of the style may be much inflated, even bulbous. Flowers of Gethyllis may have numerous stamens.
Johri et al. (1992) suggest that the embryo sac is the common monosporic 8-celled Polygonum-type, but this is questionable. Although the embryo sac of Crinum flaccidum, with ategmic ovules and nuclear endosperm, is said to be Polygonum-type, that is not confirmed by the description given; it is also conceivable that the species has parietal tissue 2-3 cells across (c.f. Howell & Prakash 1990; see also Dutt 1962). Sternbergia (Narcisseae) is reported to have a bisporic embryo sac, but this develops from the micropylar member of the dyad (Dane 1999), so is the Endymion type, while Leucojum aestivum (Galantheae) has an Allium-type embryo sac (Ekici & Dane 2005). Hymenocallis caribaea has parietal tissue, the micropyle is zig-zag and mostly made up of the very long inner intgument which is almost as long as the body of the ovule, and there is a massive, chlorophyllous, stomata-bearing, vascularized outer integument (Raymúndez et al. 2008). Embryology here needs a review.
A very long-tubular dropper cotyledonary sheath may develop during germination; this ensures that the bulb develops well below the soil surface.
For general information, see Markötter (1936: some South African taxa), Meerow and Snijman (1998) and Duncan et al. (2016, 2020: southern African taxa - spectacular images), and for anatomy, see Arroyo and Cutler (1984), for pollen, see Dönmez and Isik (2008), and for embryology, see Stenar (1925).
Phylogeny. Phylogenetic relationships within Amaryllidoideae are [Amaryllideae [Cyrtantheae [Calostemmateae, Haemantheae, Gethyllideae [Eurasian Clade [Andean Clade, Extra-Andean Clade]]]]] (Meerow et al. 1999, 2000a, 2000b; see also Ito et al. 1999). Relationships between major clades of American and some southern African members are not well understood, furthermore, Meerow et al. (2006) found that the inclusion of Hannonia, Lapiedra and Vagaria destabilised relationships in the European clade; Lledó et al. (2004) included the last two in Galantheae. Meerow and Clayton (2004) discussed relationships among African taxa. A more recent study using genes from all three compartments and sampling 108 species recovered the relationships [Amaryllideae [[Calostemmateae [Cyrtantheae + Haemantheae]] [Eurasian Clade [Andean Clade, Extra-Andean Clade]]]], although support for some nodes was poor (Rønsted et al. 2012: see classification above). Meerow et al. (2006) provide a phylogeny for the Eurasian Clade, which includes daffodills, snowdrops, etc. There the main dichotomy separates the Central and East Asian Lycorideae from the rest, which centre on the Mediterranean region. ITS and ndhF phylogenies are not congruent (Meerow & Snijman 2006). Meerow et al. (2020: nuclear and chloroplast data) discuss relationships in the Andean Clade; there is some hybridization, but it seems not to have affected the detection of major (= tribal) relationships, but note that Pamianthe tends to wander around the tree.
Amaryllideae. Meerow and Snijman (2001, see also 2006) discuss relationships within Amaryllideae; Amaryllis and Boophone are successively sister to the rest of the tribe; Amaryllis differs from other Amaryllidineae in not having a green testa, etc.. Meerow et al. (2003) outline the phylogeny of Crinum, the only pantropical member of Amaryllidaceae; see also Kwembeya et al. (2007). Cyrtantheae. For a phylogeny of Cyrtanthus and discussion on its evolution, see Snijman and Meerow (2010); molecules and cytology, but less so morphology, tend to agree, and the old species groupings, based on floral (pollinator) morphology, have broken down. Galantheae. For alkaloids and phylogeny, see Lledó et al. (2004) and Larsen et al. (2010). Haemantheae. For relationships here, see Conrad et al. (2006) and Bay-Smidt et al. (2011); Gethyllis is embedded in Haemantheae (Rønsted et al. 2012). Hippeastreae. Relationships are reticulating in many Hippeastreae-Hippeastrinae in particular, and species numbers are very uncertain (García et al. 2014, 2017, 2019). Narcisseae. For Narcissus, see Rønsted et al. (2008b: acetylcholinesterase-inhibiting alkaloids), Santos-Gally et al. (2012) and Marques et al. (2017).
Worsleya and Griffinia are morphologically and phylogenetically isolated (Meerow et al. 2000a).
Classification. For the infrafamilial classification of Amaryllidaceae, I follow Chase et al. (2009). For a classification of the Andean Tetraploid Clade, see Meerow et al. (2020), for that of Amaryllideae, see Meerow and Snijman (2001), for that of Hippeastreae, see García et al. (2019: comments on making an hierarchical classification for a group in which relationships are best represented as networks), for generic limits in Galantheae, see Lledó et al. (2004), and for an infrageneric classification of Narcissus, see Marques et al. (2017).
Botanical Trivia. The "amaryllis" of many a windowsill is really an Hippeastrum.
ASPARAGACEAE Jussieu, nom. cons. - Back to Asparagales
?Steroidal saponins; x = 9 (?8), nuclear genome [1 C] (0.403-)4.7(-36.649) pg.
153/2,595 (2,900). World-wide, but not Arctic - seven subfamilies below: Agavoideae, Aphyllanthoideae, Asparagoideae, Brodiaeoideae, Lomandroideae, Nolinoideae and Scilloideae (see also Anthericaceae, Eriospermaceae, Hyacinthaceae, Laxmanniaceae, and Ruscaceae, family names that are rather different to the subfamilial names that are also used).
Age. Divergence within the crown group began ca 89 Ma (Janssen & Bremer 2004). Eguiarte (1995: Agavaceae and Nolinaceae), however, suggested an age of only some ca 47 Ma, Bell et al. (2010) suggested a crown-group age of (66-)56, 51(-42) Ma, while estimates in S. Chen et al. (2013) are (65-)56(-48) or ca 36.4 Ma and in C. I. Smith et al. (2021) they are (90.6-)63.8(-44.7) Ma.
Evolution: Divergence & Distribution. Note that some of the ages given for nodes in this clade by S. Chen et al. (2013) are for nodes not recognized here.
There are no obvious apomorphies for Asparagaceae s.l., however, "endosperm thick-walled, pitted, hemicellulosic" might be placed at this level. The homoisoflavanones found in Scilloideae are rather uncommon in flowering plants, but they are also found in Camassia (Agavoideae, ex Chlorogaloideae) and Ophiopogon (Nolinoideae).
Phylogeny. These seven subfamilies form a rather well supported clade in Fay et al. (2000). Fay et al. (2000), Pires et al. (2001), and Pires and Sytsma (2002) discuss uncertainties as to the immediate sister taxon to Themidaceae (= Brodiaeoideae). Aphyllanthes has a very long branch in the three-gene analysis of Fay et al. (2000), and its phylogenetic position is unclear; its removal from analyses can rather dramatically changes support values (Chase et al. 2006; Givnish et al. 2018b). A position close to Hyacinthaceae (= Scilloideae) was found by McPherson and Graham (2001), but Pires et al. (2006) place it sister to Laxmanniaceae (= Lomandroideae), albeit with weak support. Seberg et al. (2012) found the relationships [[Brodiaeoideae + Scilloideae] [Aphyllanthoideae + Agavoideae]], but the position of Aphyllanthes had no support. Steele et al. (2012) also found Aphyllanthes associating with this group, but again with little support. The [Themidaceae + Hyacinthaceae] clade is moderately well supported (Fay & Chase 1996; Meerow et al. 2000), but support in the two-gene analysis of Jang and Pfosser (2002: Aphyllanthes not included) is only weak (see also Chase et al. 2006; Pires et al. 2006). Steele et al. (2012) recovered a clade [Lomandroideae [Asparagoideae + Nolinoideae]] that had good support (for this clade, see also Fay et al. 2000: moderate support; Seberg et al. 2012, strong support). A placement of Eriospermum (Nolinoideae here) as sister to Asparagoideae has quite strong support (Seberg et al. 2012); this position must be confirmed, while Eguchi and Tamura (2016) retrieved a clade [ Nolinoideae [Asparagus + Cordyline], although relationships at this level were not their focus. For more details of relationships, see also Bogler et al. (2006).
Classification. This is a highly unsatisfactory family. Nothing characterises it, and while some of the subfamilies do indeed have several distinctive apomorphies and are also easy to recognise, others are difficult to recognise. However, any way one might want to divide the group would be unsatisfactory. As it is, Nolinoideae and Agavoideae are particularly heterogeneous, several families having been segregated from them in the past. The flowers of the whole group are for the most part a rather undistinguished "lily"-type, and quite often are rather small. The subfamilial classification follows that in Chase et al. (2009b), but I also mention familial names for some (and there are links above) because the roots of the two sets of names differ in over half the cases and both will be encountered in the current literature (e.g. Eggli & Nyffeler 2020).
[Aphyllanthoideae [Agavoideae [Brodiaeoideae + Scilloideae]]: ?
Age. The age of this node is (59-)50(-41) or ca 40.5 Ma (S. Chen et al. 2013: c.f. dates for Agavoideae). If there is a clade [Aphyllanthoideae + Agavoideae], its age is estimated to be ca 47.6 Ma (Givnish et al. 2018b).
1. Aphyllanthoideae Lindley - Back to Asparagales
Flavonols +, ?saponins; root cortex sloughs off, endodermis becomes superficial, vessel elements often with simple perforation plates; monocot secondary thickening +; stems alone photosynthetic, with parallel wax scales; leaves two-ranked, scaly, non-photosynthetic, ligulate, vernation supervolute-subinvolute, base?; inflorescence scapose, flowers multibracteolate, sessile; T marcescent, basically free, with a single trace; A adnate to base of T; pollen spiraperturate; ovary sulcate down middle of loculus; infra-locular septal nectaries +, stigma trifid, dry; ovule 1/carpel, micropyle?; seeds slightly flattened, exotestal cells large, isodiametric; endosperm ?, 0; n = 16; cotyledon photosynthetic, terete, first leaf terete.
1[list]/1: Aphyllanthes monspeliensis. W. Mediterranean. [Photo - Flower © E. Bourneuf.]
Synonymy: Aphyllanthaceae Burnett
Chemistry, Morphology, etc.. The stomata are in bands down the scape. The tepals have but a single bundle. Is there chelidonic acid?
General information is taken from Conran (1998); he mentions helobial endosperm development here, but c.f. Schnarf and Wunderlich (1939), apparently the only source of embryological information.
Phylogeny. Remember that the immediate relationships of Aphyllanthoideae are unclear, although it it to be included in Asparagales.
[Agavoideae [Brodiaeoideae + Scilloideae]]: ?
Age. The age of this node is estimated at (62-)51, 46(-37)Ma by Bell et al. (2010) and at ca 49.8 or 33.5 Ma by S. Chen et al. (2013).
2. Agavoideae Herbert - Back to Asparagales
Plant rhizomatous; root exodermis often multilayered; outer integument 4-6 cells across; hypostase +; embryo sac with chalazal constriction; endosperm thick-walled, pitted, hemicellulosic.
23/637 [list: to tribes] - five groups below. More or less world-wide, esp. S.W. North America, few in Malesia, N. Australia, not cold temperate, New Zealand, etc. (map: see Ying et al. 1993; García-Mendoza & Galván V. 1995; Fl. N. Am. 26: 2002; Seberg 2007).
Age. Crown-group Agavoideae can be dated at (76-)61.5(-47.5) Ma (McKain et al. 2016c) or (53-)42.5(-34) ca 22.0 Ma (Givnish et al. 2015), ca 19.9 Ma (S. Chen et al. 2013: perhaps) or (66.5-)48.0(-31.9) ma (C. I. Smith et al. 2021). Once again\, one is pretty much left hanging.
2A. Anemarrheneae Reveal
Leaves ?spiral, base?; inflorescence subspicate, branched; T ± free; A 3, opposite and adnate to middle of inner T; ovules 2/carpel, apotropous; seeds angled; endosperm haustoria +; embryo curved; n = 11; hypocotyl 0.
1/1: Anemarrhena asphodeloides. N. China, Korea.
Synonymy: Anemarrhenaceae Conran, M. W. Chase & Rudall
[Agaveae [Behnieae [Herrerieae + Anthericeae]]]: (vessels in stem); nucellar cap, hypostase +.
Age. The age of this node is some (56-)41.5(-26.5) Ma (McKain et al. 2016c), (48-)40, 33(-23) Ma (Bell et al. 2010), 36-35 Ma (Wikström et al. 2001) or 34.2-29.1 Ma (Good-Avila et al. 2006).
2B. Agaveae Dumortier // the ABK clade [Agavoideae Bimodal Karyotype clade]
Rhizomatous, to trees, (bulbs, tunicated or not); steroidal saponins, non-protein amino acids, (homoisoflavanones - Chlorogalum), flavonols +; root exodermis multilayered/0, medulla with xylem or not; (monocot secondary thickening +); (silica bodies in bulb - Polianthes); adaxial bundles in leaf inverted [?level]; also styloids +; (stomata para- or tetracytic), cuticular wax rodlets parallel; (rhexigenetic lacunae + - Chlorogalum, etc.), leaves spiral, (pseudopetiolate), (often fleshy), (margins serrate), apex (pungent-)pointed, base ?; inflorescence usually branched, and/or flowers in pairs or fascicles, (pedicel articulated - Chlorogalum, etc.); flowers large, (monosymmetric); T ± connate; A adnate to T; tapetal cells several-nucleate; pollen semitectate, (operculate); ovary superior to inferior, (style 3-branched, with 3 canals - Camassia), stigma wet to dry; ovules many/carpel, outer integument (4-)9-14 cells across, (parietal tissue 1-2 cells across), (nucellar cap 2 cells across), ± postament, obturator +; (fruit septicidal - capsule - some Yucca), (fruit a berry), T marcescent; seeds flattened/globose, with phytomelan; (endosperm thin-walled - Hosta), (perisperm +, oily - Yucca, Agave); n = 30, karyotype bimodal [25 short + 5 long, also 7, 12, 18 S + 5, 3, 6 L], 0.4-10 µm long; genome duplication; (cotyledon non-photosynthetic - Funkia), hypocotyl to 4 mm long, collar rhizoids +, primary root often branched.
10/340 (?600): Agave (220), Yucca (50), Hosta (23). Central U.S.A. to N. South America, mostly S.W. North America, also East Asia (Hosta). [Photo - Flower.]
Age. Crown-group Agaveae are (37.5-)28(-20.5) (McKain et al. 2016c), (33.4-)25.8, 20.5(-18.4) (Good-Avila et al. 2006) or (33.4-)23.7(-14)/(15.1-)14.5(-13.3) Ma (C. Smith et al. 2008).
Synonymy: Agavaceae Dumortier, nom. cons., Chlorogalaceae Doweld & Reveal, Funkiaceae Horaninov, Hesperocallidaceae Traub, Hostaceae B. Mathew, Yuccaceae J. Agardh
[Behnieae [Herrerieae + Anthericeae]]: ?
Age. The age of this node is some (34-)24, 22(-13) Ma (Bell et al. (2010).
2C. Behnieae Reveal
± Sprawling, (dextrorsely twining stems), rhizomatous; tannin cells 0; velamen 1-layered; vessel elements also in the stem; leaves two-ranked, "supervolute", petiolate, blade broad, with midrib and transverse tertiaries, leaf base not sheathing; plant dioecious; staminate flowers: A adnate to base of T, tapetal cells binucleate, pistillode +; pistillate flowers: staminodes +; stigma 3-lobed, wet; ovules 2-3/carpel, micropyle endostomal, outer integument 3-4 cells across, parietal tissue ca 1 cell across; fruit a berry, T marcescent, not twisting; seeds angular, phytomelan 0, testa and tegmen thin-walled, (exotesta exfoliates); endosperm walls thick, pitted, aleurone +, embryo "large, capitate"; n = ?; cotyledon green.
1/1: Behnia reticulata. Zimbabwe to eastern South Africa.
Synonymy: Behniaceae Conran, M. W. Chase & Rudall
[Herrerieae + Anthericeae]: ovules 1-many/carpel.
2D. Herrerieae Baillon
Usu. climbers, prickly; saponins +, chelidonic acid?; root (exodermis multilayered); (vessel elements +); mucilage cells 0; cuticular wax rodlets parallel; leaves spiral, fasciculate, sheath?; pedicels not articulated; T and A free; parietal tissue?; fruit a septicidal capsule; seeds flattened; "embryo short"; n = 27, dimorphic [one large], chromosomes 0.7-3.7 µm long [Herreria]; "germination epigeal".
2/9. South America (Brazil southwards), Madagascar. [Photo - Fruit.]
Synonymy: Herreriaceae Kunth
2E. Anthericeae Bartling
Rhizome short; chelidonic acid +; (velamen +); (vessel elements in the stems); mucilage cells +, tannin cells 0, (styloids + - Chlorophytum); cuticular wax rodlets parallel; leaves spiral to two-ranked, base sheathing; inflorescence thyrsoid, flowers in groups along the axis, (raceme); (pedicels not articulated); (flower monosymmetric), (T tube 0); (pollen mixed with raphides); stigma dry; outer integument ca 4 cells across, parietal tissue 1-2 cells across, nucellar cap + [Leucocrinum]; embryo sac haustoria common; T persistent in fruit; seeds angular or flattened, black [?level]; tegmen?; embryo curved or angled, suspensor cells flattened; n = 7, 8, 10, 11, 13-15, etc., chromosomes 2-10(-13.8) µm long, genome duplication [Chlorophytum]; cotyledon not photosynthetic, coleoptile + [Chlorophytum]; plastid transmission biparental [Chlorophytum].
8/285: Chlorophytum (150), Anthericum (65), Echeandia (60). More or less worldwide, but not cold temperate, few in Malesia, N. Australia, not New Zealand, etc. [Photo - Inflorescence, Flower.]
Synonymy: Anthericaceae J. Agardh
Evolution: Divergence & Distribution. Good-Avila et al. (2006) suggest that Agave et al. are only some 26-20 Ma, and Yucca is younger, 18-13 Ma old. Rocha et al. (2006) suggested ca 12.75 Ma as the age of Agave etc. and ca 10.2 Ma for Agave s.l. (Hesperaloe and everything above in the tree - Bogler et al. 2006; c.f. also Smith et al. 2008); there are yet other possibilities for dates.
Good-Avila et al. (2006) discussed diversification in both Agave, which they thought was connected with the adoption of bat-pollination, and Yucca (see also Rocha et al. 2006). C. Smith et al. (2008) suggested that diversification was not significantly different in Yucca, with 34(-50) species, and its sister taxon, Agave s.l., with some 250 or more species. Pulses of diversification in agaves may have happened a mere 9-6 Ma, a time when other succulent clades were diversifying (e.g. Good-Avila et al. 2006; Arakaki et al. 2011).
Ecology & Physiology. Nobel (1988) discussed the eco-physiology of agaves and their relatives. Over 300 species are succulents, mostly leaf succulents (Nyffeler & Eggli 2010b); drought tolerance is common, and some species in the Chlorogalum area grow on serpentine soils, themselves often subject to drought (Halpin & Fishbein 2014).
The CAM photosynthetic pathway has evolved ca three times in Agaveae, a major CAM clade, and is found in nearly all species of Agave (there seems to have been a reversal in Polianthes [= Yucca] tuberosa, at least), Yucca subgenus Sarcocarpa and Hesperaloe (Heyduk et al. 2016). Interestingly, succulent leaves with a three-dimensional venation system that are characteristic of the CAM species are also found in related C3 species, and CAM morphology may have evolved before CAM photosynthesis itself (Heyduk et al. 2016), although some genes involved in CAM were also expressed there before CAM had developed (Heyduk et al. 2019).
Pollination Biology & Seed Dispersal. The Yucca-yucca moth association is well known. Yucca moths are in the genera Tegeticula and Parategeticula (Prodoxidae), a rather basal glossatan (= with proboscis) moth clade. Attracted to the yucca flower by scents in which homoterpenes, which are often also involved in plant defence, are a major component (Svensson et al. 2005), the moths mate in the flower, and the female moth lays eggs in the ovary and then puts pollen on to the stigma. The ovules are pollinated, and although some of the developing seeds are eaten by the caterpillar, the others escape that fate and mature. The ancestral condition for yucca moths may have been to eat ovaries (Yoder et al. 2010a). Species of the sister group of yucca moths, Prodoxus, eat fruits or flower pedicels, or are leaf miners, mainly on Yucca spp., but also Agave, etc., and more than one species of moth is sometimes found on the one species of plant (Pellmyr et al. 2005). Other close relatives of yucca moths eat various parts of Dasylirion and Nolina (both Nolinoideae-Nolineae), while yet other Prodoxidae are found Saxifragaceae), where they are involved in associations similar to those they have with Yucca. See also Ranunculaceae, Phyllanthaceae, Saxifragaceae, Moraceae and Caryophyllaceae for similar interactions; Hembry and Althoff (2016) and Kawakita and Kato (2017f) review diversification and coevolution in them, also other papers in American J. Bot. 103(10). 2016.
The yucca-yucca moth association has been used as a textbook example of mutualism or co-evolution, where the two partners, Yucca and Tegeticula, show reciprocal evolutionary changes (see Althoff et al. 2012 for details). The two parties are closely linked, but details of the association suggest that the links are not simple. Thus Prodoxus, not a pollinator but a specialist herbivore on Yucca, and Parategeticula, another pollinator, are also involved; all told, there are over 22 species of pollinating moths, 2-3 species of cheater moths, and over 35 species of Yucca (Althoff 2016 and references). Initial diversification in Yucca may have been in association with Parategeticula, a poor flier and now rather uncommon (Althoff et al. 2012). Pellmyr and Leebens-Mack (1999) estimated that the beginning of the association was around (51.5-)41.5(-31.5) Ma, active pollination by Tegeticula and Parategeticula beginning (44.5-)35.5(-26.5) Ma (see also Pellmyr et al. 1996, 2007; Pellmyr 2003; Gaunt & Miles 2002: association arose ca 32 Ma; Althoff et al. 2006), but there may have been another and more recent radiation of yucca moths only 3-2 Ma. Crown Yucca has also been aged at (14.5-)12.5(-11.5) Ma, the stem age at ca 20 Ma, the stem age of Hesperoyucca being (24-)16.5(-9) Ma (McKain et al. 2016c). Other estimates include diversification of Yucca 10-6 Ma, crown Yucca, i.e. excluding Y. queretaroensis which had no fixed position, being only (6.8-)6.4(-6.1) Ma (C. Smith et al. 2008), making any co-evolutionary scenarios complicated, to say the least. However, by several accounts much of the divergence in Yucca seems to have occurred before that of its main pollinator, yet only a mere 6-4 Ma, indeed, given the vagility of the moth, it is difficult to imagine how a strict (reciprocal speciation) co-evolution might work (see also Godsoe et al. 2010; Starr et al. 2014; Hembry et al. 2014). Tegeticula also pollinates Hesperoyucca, the species of the former that is the pollinator being sister to the rest of the genus, suggesting that this pollination association is pretty old, and it seems to have evolved independently of that in Yucca (Pellmyr & Leebens-Mack 1999; McKain et al. 2016c). In an early review, Feinsinger (1983) was perhaps inclined to think that reciprocal evolution was unlikely.
For the pollination biology of Agaveae, see Rocha et al. (2006); bat pollination is common in the large genus Agave and its relatives (Fleming et al. 2009). Both the ovary and fruit of Leucocrinum (Anthericeae) are below the surface of the ground (Bogler et al. 2006).
Plant-Animal Interactions. Caterpillars of the giant skippers Agathymus and Megathymus, found in Mexico and the adjacent southwest U.S.A., bore tunnels in the roots and leaves of Agave and Yucca (Warren et al. 2009).
Genes & Genomes. A genome duplication here, the CHPOα event of ca 48.7 Ma, in Agaveae involves Hesperaloe and Chlorogalum (Landis et al. 2018). For a connection between the evolution of the bimodal karyotype of Agave, Hesperocallis and their relatives with polyploidy, see McKain et al. (2011, 2016a, esp. 2012) and Halpin and Fishbein (2014). Hesperocallis has 4 long, 2 medium and 18 short chromosomes, and there are several other combinations (Halpin & Fishbein 2014; McKain et al. 2016c), but details of how bimodality interacts with polyploidy are unclear. The switch from the 25 short + 5 long chromosomes in North American Agaveae (this is a very common combination) tends to be linked with the adoption of more mesic habitats and corresponding morphological changes (McKain et al. 2016c).
At least some mitochondrial genes show an accelerated rate of change (G. Petersen et al. 2006).
Chemistry, Morphology, etc.. Agave is rich in saponins and sapogenins (Sidana et al. 2016). The raphides of Agave are hexagonal in transverse section, each with a lamellated (?unit membrane) sheath (Wattendorff 1976).
For variegation in Hosta, see Zonneveld (2007).
The flowers of Agave are shown with the median member of the outer whorl in the adaxial position (Spichiger et al. 2004). Camassia at least has single-trace tepals, Agave, etc. have three, while Hosta may have as many as 13 traces (Lin et al. 2011). The outer tepals of Herreriopsis have sac-like bases - possibly tepalline nectaries. In Hosta the stamens are sometimes inserted on the ovary. The tapetal cells of Polianthes (= Agave) are multinucleate. Germination of the pollen grain via the proximal pole has been reported in Beschorneria (Hesse et al. 2009a). Furcraea has nuclear endosperm.
Some information on Anthericeae is taken from Conran (1998); ovule morphology is apparently known from Leucocrinum alone in this group. Ubisch bodies are present in Anemarrhena, so there is probably a glandular tapetum; information for this genus is taken from Conran and Rudall (1998: confusion over stamen position) and Rudall et al. (1998b). For information about Behnia (Behnieae) and Herreria and Herreriopsis (Herrerieae), see Conran (1998); details of ovules/embryology are unknown. The leaves of Herreria and Herreriopsis are described as being cladode-like (Conran 1998) or cladodes (D. W. Stevenson in Takhtajan 1997).
See also Verhoek (1998), Judd et al. (2013) and Thiede and Eggli (2020) for general information especially on the part that has been considered Agavaceae s. str. in the past, i.e. Agave, Yucca and their immediate relatives, see also Lynch et al. (2001: c.f. Scilloideae!) and Solano et al. (2013: Polianthes anatomy), Alvarez & Köhler (1987: pollen), Fagerlind (1941b), Cave (1948, 1955, 1974: variation in endosperm development), Wunderlich (1950: also floral morphology) and di Fulvio and Cave (1965), all embryology; see also Kubitzki (1998b: Hostaceae), Speta (1998: Hyacinthaceae-Chlorogaloideae).
Phylogeny. For relationships within Agavoideae, see Pires et al. (2004) and especially Bogler et al. (2006: 2- and 3-gene analyses, the latter with more missing data, but overall the same topology). I have followed the latter - which see for details - above. Support for the subfamily as a whole is only 75%, that for the [Behnia + Herreria, etc. + Anthericum, etc.] clade 87%, and that for [Herreria, etc. + Anthericum, etc.] only 51% (and still less in the two-gene tree); however, other nodes have close to 100% support. Largely similar relationships were found by G. Petersen et al. (2006c) in their analysis of variation of four mitochondrial genes that are evolving particularly quickly here. C. Smith et al. (2008) included Hosta, etc., in their Agavaceae and excluded Anthericaceae, although support for Agavaceae so delimited was weak; that for the still broader circumscription adopted here was stronger. The [Agaveae [Behnieae [Herrerieae + Anthericeae]]] clade has 100% support in three- and four-gene trees (Chase et al. 2000a; Fay et al. 2000; Bogler et al. 2006).
The circumscription of group 4b above, Agave, etc. + Hesperocallis, or the ABK clade, corresponds to that of Agavaceae s.l. in Bogler et al. (2006). There is a fair amount of resolution of relationships around Agave and Yucca. Agave includes Manfreda, Polianthes, etc., and [Beschorneria + Furcraea] are sister to Agave s.l., e.g. Bogler and Simpson (1995), Bogler et al. (2006) and Rocha et al. (2006). The position of Yucca is unclear, but it may well be sister to that combined clade (Bogler et al. 2006; Archibald et al. 2015; McKain et al. 2016c), while Hesperocallis undulata may be sister to the whole clade (Bogler et al. 2006), although it has also been placed sister to a clade that includes many ex-Chlorogaloideae (Halpin & Fishbein 2013; see also Archibald et al. 2014, esp. 2015), i.e. [Hesperocallis [paraphyletic Chlorogalum [Camassia + Hastingsia]]], there is a well-supported [Hesperoyucca [Hesperoaloe + Schoenolirion]] clade, although exactly where it might go is unclear (see also McKain et al. 2016: sister to the immediately preceding clade), and Hosta is sister to the rest of this whole clade. Within Camassia relationships show a fair bit of resolution (Fishbein et al. 2010; Halpin & Fishbein 2013; Archibald et al. 2015). For other phylogenetic work on this group, see Eguiarte et al. (1994), Bogler and Simpson (1996: molecular) and Sandoval (1995: morphological).
Classification. The broad concept of Agavoideae adopted here may not seem very satisfactory, but none of the alternative solutions is any better. Agave should probably include Polianthes, Manfreda, etc.; Thiede et al. (2019) provide an infrageneric classification.
Previous Relationships. Paradisea (ex Asphodelaceae/Xanthorrhoeaceae-Asphodeloideae) belongs to the Anthericeae above (e.g. Chase et al. 2000b). Behnia (Behnieae) was included in Luzuriagaceae (Liliales here) by Taktajan (1997), but it has also been placed in other lilialean and asparagalean families (Bogler et al. 2006); Camassia, etc. (Agaveae), used to be in Liliaceae (Cronquist 1981) or Hyacinthaceae-Chlorogaloideae. Traub (1982) noted that Hesperocallis undulata (Agaveae) smells of onions, and he even associated it with his Alliales. The genus was geographically odd in Hostaceae s. str., which is where other workers had placed it (c.f. Kubitzki 1998b), but not in Agavoideae as here circumscribed; now it is Hosta that is a little odd from the geographical point of view. Patil (2015) included four unrelated groups in his Agavaceae.
Botanical Trivia. The inflorescences of Furcraea might be the longest of those of any plant (Mauricio Bonifacino pers. comm. - horse for scale), although in terms of mass and flower number, Corypha (Arecaceae) is the largest.
[Brodiaeoideae + Scilloideae]: leaves spiral; inflorescence scapose, pedicels bracteate; raphides in carpel wall; ovules anatropous; endosperm (nuclear); cotyledon not photosynthetic.
Age. The age of this node is estimated at (56-)45, 40(-15)Ma by Bell et al. (2010) and at (58-)48(-40) or around 40.6Ma by S. Chen et al. (2013).
Evolution: Divergence & Distribution. For some other characters of this pair, see Fay and Chase (1996); laticifer-like structures may occur in both.
3. Brodiaeoideae Traub - Back to Asparagales
Plant monopodial, cormose, storing starch; root pith 0; laticifers +; mucilage cells?; leaves (unifacial - Brodiaea), sheath closed, fibrous; inflorescence umbellate, cymose, inflorescence bracts several, scarious, also internal bracts; pedicels often articulated; (T free; corona +); A (3), connate and/or adnate to T, (filaments flattened); (ovary stipitate, adnate to T by flanges opposite the outer tepals), stigma capitate to trifid, dry (wet - Bloomeria); ovule with outer integument 3-4 (5-7 - Dichelostemma) cells across, (inner integument 3+ cells across), parietal tissue 3-4 cells across, (nucellar cap +); seeds angular, cells of tegmen much enlarged (not - Triteleia); "embryo short"; n = 5-12+; hypocotyl?, primary root persistent.
12[list]/62: Brodiaea (14). S.W. North America, to British Columbia and Guatemala (map: see H. E. Moore 1953; Fl. N. Am. 26: 2002). Photo: Flower, Flower, Fruit.
Age. Divergence within Brodiaeoideae began around 25.1 or (26-)20(-24) Ma (S. Chen et al. 2013).
Synonymy: Themidaceae Salisbury
Chemistry, Morphology, etc.. Little is known about the chemistry of Brodiaeoideae.
When the tepalline tube is adnate to the stipitate gynoecium, three narrow, ?nectar-containing tubes are formed. Embryologically Brodiaeoideae are quite variable. The inner integument is massive or not, ditto base of the nucellus, endosperm development varies, etc. (Berg 1978, 2003 for a summary).
Some information is taken from Rahn (1998: general) and H. E. Moore (1953: morphology).
Phylogeny. There are two major clades, [Muilla, Triteleia] and [Dipterostemon, Dichelostemma, Brodiaea], albeit with only moderate support. The first clade has a long tepalline tube and the second has appendages on the bases of the filaments that form a nectar cup; both characters arise in parallel in the two clades (Pires & Sytsma 2002; c.f. Seberg et al. 2012). See also Pires et al. (2001) for phylogeny and morphological evolution.
Previous Relationships. Themidaceae/Brodiaeoideae have often been included in Alliaceae/Amaryllidaceae-Allioideae because of their superficially similar umbellate inflorescence and rather undistinguished monocot flowers (e.g. Takhtajan 1997).
4. Scilloideae Burnett - Back to Asparagales - needs reworking.
Plant bulbous, geophytic, roots often contractile; endomycorrhizae 0; polyhydroxyalkaloids, homoisoflavones, flavone C-glycosides +; root contractile, exodermis 1-layered; leaf with little (well developed) sclerenchyma, mucilage cells +; (leaf waxes with parallel platelets); bulb leaf sheaths closed or not; inflorescence scapose [?all], (branched), (spike), pedicels not articulated, bracteole 0; (corona +); stigma capitate to punctate and papillate; ovules 1-many/carpel, outer integument 2-4 cells across, parietal tissue 1-4 cells across, (nucellar epidermis radially elongated), nucellar cap +/0, hypostase +, raphides +, obturator +; seeds black; testa multi-layered; chromosomes 1.2-18 µm long; nucleus with protein crystals; (hypocotyl 0; collar rhizoids +).
41-70 [list, to tribes]/800-1025 - six groupings below. Predominantly Old World in Mediterranean climates, esp. S. Africa and the Mediterranean, to Central Asia and Japan; a few in South America (map: both colours).
Age. Oziroë diverged from the rest of the clade in the Oligocene ca 28 Ma (Ali et al. 2012).
4A. Oziroëeae M. W. Chase, Reveal & M. F. Fay
Flowers (1-)2(-3)/bract; A basally connate and adnate to C; stigma punctate; seeds rounded, surface rugose; embryo long; n = 15, 17; cotyledon?
1/5. Western South America. Map: see above, green, from Guaglianone and Arroyo-Leuenberger (2002).
[Ornithogaleae + Urgineeae + Hyacintheae]: fructan sugars accumulated; root stele narrow, not medullated, with a central vascular element; rhexigenetic lacunae +; also styloids +; (pollen mixed with raphides); (antipodal cells polyploid).
Age. The beginning of divergence within this clade can be dated to (47-)37(-29) or around 25.2 Ma (S. Chen et al. 2013).
4B. Ornithogaleae Rouy
Cardenolides +; (root stele with several central vascular elements); T multinerved; A (3), (filaments flat, with appendages); tapetal cells 2-5-nucleate; stigma 3-lobed/capitate; antipodal cells persist in pouch of embryo sac; seeds flattened/angled; n = 2-10+, nucleus with protein crystals; cotyledon photosynthetic or not.
4/312: Ornithogalum (160), Albuca (110-140). Europe, W. Asia, Africa.
Synonymy: Ornithogalaceae Salisbury
4C. Urgineeae Rouy
(Plant climbing); bufadienolides +; root stele with several central vascular elements; bracts spurred-peltate [as small leaves in Bowiea], bracteoles usu. 0 (1, ?2); flowers usu. short-lived; T (free - Bowiea), outer whorl with 5 traces, inner whorl with 3; A with two bundles in filaments [Drimia], anthers (porose); (stylar canals 3 - Boweia), stigma ± capitate/lobed; capsule ± abruptly narrowed at apex, (T persistent - Bowiea); seeds angled/flattened-winged; testa brittle, not tightly adherent to endosperm; n = 6, 7, 10+ [x = 10], karyotype bimodal, nucleus without protein crystals.
2/111: Drimia (110). Mainly southern Africa, also Madagascar and the Mediterranean to India (map: from Pfosser & Speta 2001). Photos: Boweia Collection.
4D. Hyacintheae Dumortier
Homoisoflavanones +; root (stele with several central vascular elements/medullated); (leaves with pustules or coloured spots); T with a single trace; stigma feathery; parietal tissue +; embryo sac variable, e.g. bisporic (the chalazal dyad) [Allium-type]/8-celled bisporic (the micropylar dyad) and 8 celled [Endymion-type]/monosporic, 8-celled [Polygonum type]; seeds (brown to yellow), usu. rounded, elaiosomes common.
Age. Crown Hyacintheae are ca 18.8 Ma (Ali et al. 2012).
a. Pseudoprosperinae J. C. Manning & Goldblatt
Root stele?; (inflorescence branched); bracteoles +, ± lateral; 2 ovules/carpel; 1 seed/loculus; n = 9; cotyledon not photosynthetic.
1/1: Pseudoprospero firmifolium. Southeast South Africa (Map: blue-green).
[Massoniinae + Hyacinthinae]: ?
Age. The age for this node is ca 17.9 Ma (Ali et al. 2012).
b. Massoniinae Bentham & J. D. Hooker
(Bracteoles +); leaves (pseudopetiolate); T one- or multinerved; (flowers monosymmetric); A basally connate; ovary and style sulcate, style with 3 canals; ovules 2-many/carpel); (suprachalazal tissue long, with central column of cells - Drimiopsis [= Ledebouria]); testa (ruguse/puberulous/echinulate), (elaiosomes +); n = 5-10+, many 20 [x = 10]; cotyledon not photosynthetic (photosynthetic).
Ca 10/260: Lachenalia (135), Ledebouria (70). Africa S. of the Sahara, Ledebouria to India (map: above, from Venter 2008, red, including blue-green area).
Age. Crown Massoniinae are ca 16.3 Ma (Ali et al. 2012).
Synonymy: Eucomidaceae Salisbury, Lachenaliaceae Salisbury
c. Hyacinthinae Parlatore
Endomycorrhizae +; (bracts 0), bracteoles quite common; stylar canal papillate; ovules 2-8(-many)/carpel, (outer integument 4-5 cells across), antipodal cells large; seed (elaiosomes +); embryo suspensor filamentous; n = 4-8+ [x = 9]; cotyledon photosynthetic or not.
21/265: Muscari (50), Bellevalia (50), Scilla (30), Prospero (25, ?= Scilla). Europe (not the northeast), the Mediterranean, the Mid East, North Africa, Barnardia [= Scilla] japonica in the Far East (map: Meusel et al. 1965). [Photo: Scilla Collection.]
Age. Crown Hyacinthinae are ca 15.3 Ma (Ali et al. 2012).
Synonymy: Hyacinthaceae Borkhausen, Scillaceae Vest
Evolution: Divergence & Distribution. Hyacintheae may have originated in sub-Saharan Africa and dispersed north and also east, but details depend on the analytic method used (Ali et al. 2012). There are about 300 species of Scilloideae in the Cape flora alone (Procheŝ et al. 2006), about 400 species in southern Africa (Johnson 2010).
Ecology & Physiology. Many species in the foggy deserts of Namaqualand, South Africa, have water-catching leaves with very distinctive morphologies (Vogel & Müller-Doblies 2011).
Pollination Biology & Seed Dispersal. Lachenalia has monosymmetric flowers in which the median member of the outer whorl is in the adaxial position. The same is true of the remarkable monosymmetric flowers of Massonia (Daubneya) aurea that are on the outside of the inflorescence. These flowers have the three abaxial tepals greatly enlarged, while the inner flowers are polysymmetric, the tepals forming a simple, lobed tube: The result is an inflorescence looking like a flower. Pollination in Albuca is noteworthy in that the pollen is deposited by leaf-cutter bees on the tips of the inner tepals, but pollination is not completed until two to three days later when the flower withers, the tepals then press against the stigma, and the pollen finally germinates (Johnson et al. 2009b, 2012).
Species with myrmecochorous seeds are scattered throughout the subfamily (Lengyel et al. 2010).
Vegetative Variation. Some species of Scilloideae have terete, unifacial leaves, as in Ornithogalum, where they develop from the upper part of the leaf (Kaplan 1973). Even the bulb scales of some species of Rhadamanthus (= Drimia) are terete. Urgineeae have a backwardly-directed process at the base of the leaves and/or bracts (c.f. Asparagus-Asparagoideae). Vegetative variation - in both leaf and bulb - is also considerable in Ledebouria (Venter 2007). However, there is less anatomical variation.
Genes & Genomes. High C values in Scilla are associated with long cell cycles, as has been noticed elsewhere (Francis et al. 2008). For the cytology of some sub-Saharan members of the subfamily, see Goldblatt and Manning (2011); Goldblatt et al. (2012) suggest base numbers for tribes, etc.. Karyotypes may be bi- or even trimodal.
Chemistry, Morphology, etc.. Bufadienolides are cardiac glycosides. Although mucilage cells are particlarly common in Scilloideae, they also occur elsewhere (Lynch et al. 2006). The vascular bundles in the scape of Drimia are endarch (Carpenter 1938),
Some Scilloideae have a filament tube. Wunderlich (1937) described the endosperm as being both helobial and nuclear in Hyacinthineae. The leaves of seedlings are two-ranked.
Information is taken from Speta (1998b: general, 2001: subfamilial characters), Pfosser and Speta (1999), Manning and Goldblatt (2018: Urgineeae) and van Jaarsveld and Eggli (2020b: Hyacinthaceae); for chemistry, see Kite et al. (2000), Pfosser and Speta (2001) and Koorbanally et al. (2008), for anatomy, see Lynch et al. (2001: leaf) and Sobotik and Speta (1997: root), for floral morphology in Ledebouriinae, see Lebatha and Buys (2006), for floral vasculature, see Carpenter (1938) and Deroin (2014), for embryology, very variable, see Sundar Rao (1940), Eunus (1950a), von Guttenberg and Jakuszeit (1957: Galtonia, polyembryonic), Berg (1962), Chennaveeraiah and Mahabale (1962), Svoma and Greihuber (1988, 1989), Ebert and Greilhuber (2005) and Dane (2006) and for seed morphology, also variable, see Brudermann et al. (2018, 2019).
Phylogeny. The topology [Oziroëeae [Ornithogaleae [Urgineeae + Hyacintheae]]] has moderate support in Manning et al. (2004); Oziroë and Albuca (Ornithogaleae) were successively sisters to the rest at the base of Scilloideae in Seberg et al (2012), the position of the latter genus having only moderate support. There is little well-supported structure along the backbone of Hyacintheae and again within Hyacinthineae in the trnL-F spacer analysis of Wetschnig et al. (2002); the positions of Ornithogaleae and Urgineeae were also unclear. See also Pfosser et al. (2003, 2012), the latter dealing with relationships of the Malagasy taxa.
Classification. For a classification, see Speta (1998a: as Hyacinthaceae). However, there is considerable disagreement over generic limits here; are there 15 or 45 genera in sub-Saharan Africa? (e.g. Stedje 2001a, b; Pfosser & Speta 2001; Lebatha et al. 2006; Martínez-Azorín et al. 2015, 2019; Crouch et al. 2018). Speta (1998a) dismembered Scilla and Martínez-Azorín et al. (2011) latter broke up Ornithogaleae - 19 genera, of which 11 replace Ornithogalum; recognizability of taxa is not the issue. Manning et al. (2004) provide a generic synopsis of the family in sub-Saharan Africa that integrates some morphology with relationships; like them, I take a generally broad view of genera. However, there are unresolved issues that include sampling, whether or not floral syndromes distort ideas of relationships (and so what effect characters taken from these syndromes have in combined analyses), the consequences of maintaining well-known generic names like Albuca and Galtonia as our knowledge of phylogeny becomes clearer, and the role cytological data should play in generic delimitations. Albuca is recognized in the reclassification of Ornithogaloideae by Manning et al. (2009). Manning and Goldblatt (2018; see also Manning 2019) take a broad view of Drimia (followed here) but provide an infrageneric classification - 19 sections for the 70 southern African species, a majority of the genus, and another one for taxa from Madagscar. Manning (2020) revised the subtribal classification of Massonieae.
Previous Relationships. Chlorogaloideae, until recently included in Hyacinthaceae/Scilloideae (e.g. Pfosser & Speta 1999), are here included in Agavoideae.
[Lomandroideae [Asparagoideae + Nolinoideae]]: pedicels articulated; fruit a capsule; endosperm thick-walled, pitted, hemicellulosic.
Age. For the age of this node, estimated at (59-)49, 45(-35) Ma, see Bell et al. (2010); (60-)50(-42) or around 32.7 Ma are the estimates in S. Chen et al. (2013) and (70.3-)56.6(-45.3) Ma those in Gunn et al. (2020).
Evolution: Genes & Genomes. The LOLOα duplication, ca 68.3 Ma, can be placed at this node (Landis et al. 2018: Lom. Asp.).
5. Lomandroideae Thorne & Reveal - Back to Asparagales
(Naphthoquinones +); (vessel elements in leaves); (T connate basally), nucellar epidermal cells enlarged, supra-chalazal zone long, with central elongated cells; antipodal cells large; T persistent in fruit; seeds rounded to angular; cotyledon photosynthetic or not, (coleoptile +; first leaves reduced).
12 [list]/186 (+ 15 to be named). Madagascar, India, South East Asia to the Pacific, and South America, predominantly Australian (Map: see Schlittler 1951).
Age. The crown group age of this clade is (57-)47(-39) or around 32.7 Ma (S. Chen et al. 2013) or (60.6-)52.7(-43.7) Ma (Gunn et al. 2020).
[Lomandreae + Sowerbaea group]: flowers long-lived; T whorls at most slightly differentiated; infra-locular septal nectaries +.
Age. This clade has a crown-group age of (52.6-)41.4(-43.7) Ma (Gunn et al. 2020).
5Aa. Lomandreae Engler
Plant ± rhizomatous; root tubers 0; (monocot secondary thickening +); leaf blade with sclerenchymatous ribs extending from the inner sheath of the vascular bundle to the surface, outer bundle sheath with enlarged cells; leaves two-ranked, flat or curved, (margins with spines), (base auriculate); (plant dioecious - Lomandra); pedicels articulated; inflorescence units cymose [?all]; flowers long-lived; (pollen grains spiraperturate/irregularly syncolpate); stigma wet; ovules 1-2/carpel, nucellar cap +; testa lacking phytomelan, thin, tegmen brown, collapsed, cellular; endosperm hemicellulosic; n = 7-10, chromosomes 2-7 µm long.
4/67: Lomandra (50). Australia, New Guinea, New Caledonia (Map: Fl. Australia vol. 46. 1986; Australia's Virtual Herbarium xi.2014). [Photo - Inflorescence © K. Stüber.]
Age. Crown group Lomandreae are (34.5-)24.0(-15.0) Ma (Gunn et al. 2020).
Synonymy: Lomandraceae Lotsy
5Ab. Sowerbaea group
Plant caespitose or rhizomatous, (stilt-rooted); (roots tuberous); leaves terete to triquetrous; inflorescence scapose (sessile), capitate to umbellate; (A 3, opposite inner T; staminodes 3 or 0 - Sowerbaea), (inner A adnate to T); stigma dilated or punctate; ovules 1-8/carpel; seeds dull brown to black, no aril, etc.; n = 4.
2/18: Laxmannia (13). Southern Australia.
Age. The crown group age of this clade is (40.1-)29.1(-19.3 Ma (Gunn et al. 2020).
Synonymy: Laxmanniaceae Bubani
[Arthropodium group + Cordylineae]: flowers open one day [check]; nectary 0; testa with phytomelan.
Age. The crown group age of this clade is (55.2-)47.4(-40.0) Ma (Gunn et al. 2020).
5B. Arthropodium group
Plant (annual), (rhizomatous), (climbing); (ecto)/vesicular-arbuscular mycorrhizae; roots often tuberous; (monocot secondary thickening + - Thysanotus); mucilage +; leaves spiral, vernation supervolute or conduplicate, (petiolate), (ligulate); flowers single or in groups, pedicel articulated or not; P whorls well differentiated, inner T long fimbriate/with hairy margins (not); (A 3), anthers dehiscing by pores (not - Trichopetalum)), (filaments with dense tufts of hairs [if inner T are not barbate]); stigma wet; seeds often arillate (strophiolate); exotesta often papillate, rest of testa cellular, tegmen thin; endosperm thin-walled; n = 9-11, chromosomes 0.5-2 µm long.
6/74: Thysanotus (50), Arthropodium (20). South East Asia to Australia, New Zealand and the Pacific, Madagascar, C. Chile, Neuquén Province, Argentina. (Map: Fl. Australia vol. 45. 1987; vol. 46. 1986; Schlittler 1951; Fl. China vol. 24. 2000; Australia's Virtual Herbarium xi.2014).
Age. The crown group age here is (46.3-)36.6(-26.7) Ma (Gunn et al. 2020).
Synonymy: Eustrephaceae Chupov
5C. Cordylineae Nakai
Rosette herbs to trees; storage roots +; fructan sugars accumulated; monocot secondary thickening +; mucilage +; stomata paracytic, subsidiary cells with oblique divisions, amphistomatouis; leaves spiral, vernation supervolute or conduplicate, (pseudopetiolate); flowers single along axis, pedicel articulated, short; fruit a berry; testa anatomy?; endosperm ?; n = 19, chromosomes 0.5-2.4 µm long.
1/17. Mascarenes, northeast Australia, New Guinea to the West Pacific and New Zealand, southeast South America. (Map: Fl. Australia vol. 45. 1987, vol. 46. 1986.) [Photo - Habit, Flower.]
Age. The crown group age of Cordylineae is (25.4-)22.0(-20.0) Ma (Gunn et al. 2020).
An Eocene fossil, Paracordyline aureonemoralis, from Adelaide is rather like members of the extant Cordyline stricta/C. fruticosa complex, and that genus is also known from somewhat younger (Oligocene) deposits on Kerguélen Island (Conran & Christophel 1998).
Evolution: Bacterial/Fungal Associations. See Brundrett (2017a) and Tedersoo and Brundrett (2017) for the distinctive mycorrhizal association formed by the Australian Thysanotus. Fungi are associated with the subepidermal layer of cells (McGee 1988).
Chemistry, Morphology, etc.. There are reports of cell wall ferulates from Xerolirion (Rudall & Caddick 1994), which, if confirmed, would make it about the only non-commelinid genus with them.
The trunks of Cordyline develop massive aerial roots after injury, rather like those of Dracaena (Krawczyszyn & Krawczyszyn 2014). Eustrephus has vessels in its leaves. The leaves of Lomandra and its relatives have sclerenchymatous ribs extending from the inner sheath of the vascular bundles (c.f. also Cordyline?: Rudall & Chase 1996).
Xerolirion has solitary, terminal carpelate flowers, while its staminate flowers are in cymes. The pollen of Lomandra is very variable, sometimes being spiraperturate (c.f. Aphyllanthes). There is considerable variation in seedling morphology, even within individual groups (Conran 1998).
Additional information is taken from Chase et al. (1996), Conran (1998, as Lomandraceae), general, Schlittler (1951: Eustrephus), Chanda and Ghosh (1976: pollen, as Xanthorrhoeaceae) and Rudall (1994b, 2000: ovule, etc.).
Phylogeny. McLay and Bayly (2016) found two well supported clades in Lomandroideae. One included the [Chamaexeros + Lomandra] clade, with [Sowerbaea + Laxmannia] as its sister, the other was the [Trichopetalum, Arthropodium, Murchisonia] clade, and here Cordyline may be sister to the rest. Relationships found by S-C. Chen et al. (2013) are similar, as are those suggested by Gunn et al. (2020: sampling good). The latter found Trichopetalum to be well supported as sister to the rest of the Arthropodium clade (hence anther dehiscence is not likely to be an apomorphy for it), and Arthropodium itself was paraphyletic. A paraphyletic Lomandra, including Xerolirion, was sister to other Lomandreae (Gunn et al. 2020).
For the Cordyline group, see Chase et al. (1996), and for relationships in Thysanotus, see Sirisena (2010).
Classification. I have tentatively recognised three groups above, based partly on morphology and partly on molecular data.
Previous Relationships. Chamaescilla has been moved from Lomandroideae to Asphodelaceae-Hemerocallidoideae (McLay & Bayly 2016).
The leaves of Lomandra, etc., with their sclerenchymatous ribs extending from the inner sheaths of the vascular bundles, differ from those of Dasypogonaceae (Arecales), with which Lomandra and co. were previously associated, but where this sheath is absent, and Xanthorrhoea (Asphodelaceae, see above), where the sheath develps from the mesophyll. However, the leaves of all three are xeromorphic and superficially similar (Rudall & Chase 1996).
[Asparagoideae + Nolinoideae]: steroidal saponins +; fructan sugars accumulated; (velamen +); flowers rather small[!]; T with a single trace; (fruit a berry).
Age. The age of this node is estimated at (55-)44, 42(-34)Ma by Bell et al. (2010) and at (57-)47(-37) or about 27.8Ma by S. Chen et al. (2013).
Chemistry, Morphology, etc.. For ovule development, see Rudall (1994b).
Baccate fruits containing seeds that lack phytomelan are common here, but I do not know where they might be apomorphic. The capsular Hemiphylacus and Eriospermum are respectively sister to other Asparagoideae and Nolinoideae, and baccate fruits are probably derived several times (c.f. Judd et al. 2007) - or vice versa.
6. Asparagoideae Burmeister - Back to Asparagales
Rhizome +, horizontal or vertical; flavonols, saponins +; root (velamen +); leaves spiral; pedicels articulated; nucellar epidermal cells enlarged, persistent; embryo sac curved; seed rounded to ± angled, black, with phytomelan; embryo long, slightly curved.
2[list]/175-305. Old World, also Mexico (map: from Hernandez S. 1995; Hultén & Fries 1986; FloraBase 2007; Seberg 2007; Kubota et al. 2011; B. Ford pers. comm. 2011; Trop. Afr. Fl. Pl. Ecol. Distr. 7. 2012: ?Malesia).
Age. Divergence within crown-group Asparagoideae began (25-)16(-9) or some 9.6 Ma (S. Chen et al. 2013).
6a. Asparagus L.
Herbaceous to shrubby, often climbers, rhizome +, horizontal or vertical, root tubers +/0; flavonols, saponins +; root (velamen +), exodermis multilayered; vessel elements in roots often with simple perforation plates, vessels also in stem; cuticular wax rodlets parallel; leaves reduced, (scarious), (spiny), cladodes +, flattened and foliaceous or terete; plant (mon- or dioecious); inflorescence ± fasciculate/(flowers single); T free/basally connate; A free/(basally adnate to T)/(connate); G (slightly stipitate), stigma wet or dry; ovules 1-12/carpel, tapetal cells 4-nucleate; ovule with outer integument ca 6 cells across; embryo sac asymmetric, caecum basal, no nuclei, antipodal cells lateral, dividing; fruit a berry; testa multiplicative, collapsing, exotesta massive, (exfoliating), tegmen inconspicuous; endosperm cells thick-walled, pitted, hemicellulosic; n = 10, chromosomes 1-3 µm long.
1/170-300. Old World, but only N. Australia in the Antipodes (map: see above). [Photo - Flower, Fruit.]
6b. Hemiphylacus S. Watson
Rosette-forming, (contractile roots +); leaves linear; inflorescence scapose, branched; (A 3, opposite inner T, + 3 staminodes), filaments in anther pocket; G stipitate, opposite inner T; ovules 3-6/carpel, outer integument ca 6 cells across, funicular obturator +; fruit a loculicidal capsule; testa multiplicative, collapsing, exotesta massive, tegmen inconspicuous; endosperm cells thick-walled, pitted, hemicellulosic; n = 56, chromosomes 0.7-1.7 µm long.
1/5. Mexico (map: see above).
Synonymy: Hemiphylacaceae Doweld
Evolution: Divergence & Distribution. Fukuda et al. (2005a) and Norup et al. (2015) discuss diversification in Asparagus; this seems to have been rapid and to have started in southern Africa with several subsequent independent dispersal events to the north. Asparagus is quite often found in drier/sandy habitats.
Pollination. Hybridization between species is quite common in the dioecious subgenus Asparagus (Kubota et al. 2011); dioecy seems to have evolved once in Asparagus, (Norup et al. 2015), but connections with genome duplication events are unclear (Harkess et al. 2017). Species of Asparagus with flattened cladodes have perfect flowers (Kubota et al. 2011).
Vegetative Variation. There has been much discussion as to what the more or less leaf-like structures in the axils of the leaves in Asparagus "are" - stem or leaf or something else? (see e.g. Arber 1924b - prophyllar, axial; Cooney-Sovetts & Sattler 1986 - homeotic). Nakayama et al. (2012, see also Nakayama et al. 2010) looked at the development of both leaf-like and terete cladodes in Asparagus. The former (A. asparagoides) had an inverted (= prophyllar) orientation, while the latter (A. officinalis) were ventralised (c.f. Allium). They noted that both "leaf" and "stem" genes were expressed in the cladodes; the gene regulatory network for leaf development had been coopted by the axillary shoot (Nakayama et al. 2013). The lower stem leaves and the leaves subtending the main branches are odd enought, peltate, and/or spiny, etc..
Genes & Genomes. Harkess et al. (2017, 2018/20 and references; see also Henry et al. 2018) discuss the recent evolution of a two-gene dioecy system in Asparagus officinalis. This is an XY system, but the chromosomes are indistinguishable; the Y chromosomes have a closely linked pair of genes, one promoting the male function and the other suppressing the female function.
There may have been a genome duplication around here (Harkess et al. 2017; Zwaenepoel & Van de Peer 2020).
Chemistry, Morphology, etc.. Methyl mercaptans are known from Asparagus. Mucilage polysaccharides in the roots may have a storage role.
The prophylls ("bracts") at the bases of the pedicels in Hemiphylacus are described as being lateral (Hernandez S. 1995). For floral development in Asparagus, see Park et al. 2(003, 2004); b-class genes are not expressed in the outer tepal whorl.
Some information is taken Malcomber and Demissew (1993: Asparagus) and Kubitzki and Rudall (1998), both general, Venkateswarlu and Raju (1958: embryology) Robbins and Borthwick (1925: ovule and seed) and Rudall et al. (1998b: embryology).
Phylogeny. For phylogenetic relationships in Asparagus, see Fukuda et al. (2005b), Kubota et al. (2011) and Saha et al. 2016: (subgenus Protasparagus); subgenus Myrsiphyllum, at least, is probably paraphyletic. Norup et al. (2015) found six main clades within Asparagus as well as two small clades, but relationships between these groups were not well supported.
Previous Relationships. Hemiphylacus used to be placed in Asphodelaceae-Asphodeloideae.
7. Nolinoideae Burnett - Back to Asparagales
Flavonols, (azetidine-2-carboxylic acid [non-protein amino acid]), (indolizidine alkaloids), saponins +; (velamen +); (vessel elements in roots with simple perforation plates; (vascular bundles amphivasal); cuticular wax rodlets parallel; pedicels articulated; nucellar cap 0; seed phytomelan 0; chromosomes 0.5-19 µm long; radicle well developed.
26[list: to tribes]/590 - 7 tribes beow, not all species included yet. N. hemisphere, esp. South East Asia, Africa, esp. south of the Sahara (map: from Meusel et al. 1965; Hultén & Fries 1986; Perry 1994, incomplete).
Age. Divergence within Nolinoideae began (53-)41(-31) or ca 23.6 Ma (S. Chen et al. 2013).
7a. Eriospermeae Reveal
Plant tuberous (rhizomes/stolons); ?chemistry; root medulla 0; raphides ?0; plant hysteranthous, leaves single (synanthous, leaves a few); leaves amphistomatous, no structural sclerenchyma, spiral, with sheath/pseudopetiolate, blade linear to cordate or peltate, (margin undulate), (enations + [stellate/long-penicillate/much branched (lamina proper ± 0)/etc.]; inflorescence scapose, (1 basal leaf-like inflorescence bract); bracteoles ?0; T basally connate; A adnate to base of T, anthers usu. dorsifixed, versatile; microsporogenesis successive; stigma punctate/slightly lobed; ovules 3-6/carpel, parietal tissue ca 1 layer thick, hypostase +, placental obturator +; parietal tissue 1 cell across; fruit a loculicidal capsule; exotestal cells long-hairy, meso/endo testa with phlobaphene/empty, tegmen ± collapsed, endotegmen initially tanniniferous; endosperm nuclea, 0, perisperm + [at the radicular end], embryo very large [the length of the seed]; n = (5-)7(9, 10, 12, etc.); cotyledon unifacial, photosynthetic, ring of hairs, radicle unbranched, tuber hypocotylar.
1/100: Eriospermum. Africa S. of the Sahara (Eriospermum abyssinium Senegal to Ethiopia, then south), not the Congo forest, etc,), esp. S.W. Africa and the Cape. Photograph: flower, © M. Elvin.]
Synonymy: Eriospermaceae d'Orbigny
[Nolineae + the rest]: root medulla with xylem and/or phloem, or neither; raphides +; outer integument 2-8 cells across, parietal tissue (0-)1-3(-4) cells across, nucellar cap 0 (+), (chalazal vascular bundle branched); (embryo sac bisporic, 8 nucleate [Allium type]; tetrasporic, 16-nucleate [Drusa type]), (antipodal cells numerous, persistent); radicle branched or not.
7b. Nolineae S. Watson
Plant usu. little-branched and ± tree-like, (base swollen/leaves persistent/no trunk, rosette plants); (monocot secondary thickening +); vessel elements also with simple perforation plates [lf. root, not stem]; raphides?; cuticular wax with platelets, stomata in grooves, para-/tetracytic; leaves spiral, linear, isobilateral, margins usu. serrate; inflorescence branched; plant dioecious/polygamo-dioecious; ovary 1- or 3-locular; ovules 2/carpel, basal, embryology unclear; (embryo sac haustorium - Dasylirion); fruit indehiscent, dry, ± 3-winged [1-seeded]/inflated/other; n = (18) 19.
4/52: Nolina (23). Mexico, also Central America and (S)/S.W. U.S.A..
Synonymy: Nolinaceae Nakai
7. Polygonateae Bentham & J. D. Hooker
Plant rhizomatous (epiphytic) herbs; (cardenolides + - Polygonatum); stem leafy, leaves 2-ranked, (opposite, whorled), blade broad, base not sheathing; inflorescences axillary, bracts +/0; T (imbricate - Disporopsis), connate; A adnate to T, (corona at base of filament - Disporopsis); ?septal nectaries, stigma capitate to lobed; ovules (2-)4-6(-12)/carpel; fruit a berry; n = 9-16, 20.
3/95: Polygonatum (75). N. Temperate, esp. China and adjacent areas.
Synonymy: Polygonataceae Salisbury
Plant rhizomatous; blade broad, base barely sheathing; inflorescences terminal, racemose; flowers (2-merous); T (with three traces - Smilacina s. str.); n = 18. Maianthemum (35). N. Temperate, esp. China and Cantral America. Comospermum - two tenuinucellate apotropous ovules/carpel, n = 20.
7. Convallarieae Dumortier
Plant monopodial, rhizomatous herbs; (cardiac glycosides/cardenolides - Convallaria, Speirantha); root (velamen +), (cuboidal styloids +); leaves 2-ranked/spiral; inflorescences axillary, scapose, (densely) spicate (racemose), (single flower - Aspidistra); (bracteole lateral - Rohdea); flowers (2-13 merous); T often fleshy, ± connate, (corona/annulus below A +); A adnate to base-middle of T, filaments 0-short (long exserted); G (1), ?septal nectaries, style long-slender/massive/0, stigma punctate/3-lobed/peltate-fungiform (esp. Aspidistra); ovules (1-)2-4(-many)/carpel; fruit a berry (drupe); seeds (fleshy); n = 19.
6/210: Aspidistra (170), Tupistra (20), Rohdea (17). Largely South East Asia to Sumatra, Convallaria also S.E. U.S.A and Europe.
Synonymy: Aspidistraceae Hasskarl, Convallariaceae Horaninow, Tupistraceae Schnizlein
7. Ophiopogoneae Voigt
Rhizomatous herbs; (cuboidal styloids +); leaves spiral, blade narrow, (blade, pseudopetiole +); T free to connate 50%; A (connate as corona - Peliosanthes), free to adnate to T, filaments short to long; G (subinferior), ?septal nectaries, (placentation basal), style (short to) long, stigma ± capitate; ovules 1-6/carpel; fruit a berry; (seed exposed early in development, testa fleshy - Liriope); n = 18, 2C = 8.62-24.65 pg.
3/145: Ophiopogon (67), Peliosanthes (60). Mostly (warm) temperate South East Asia, the Philippines, esp. China.
Synonymy: Ophiopogonaceae Meissner, Peliosanthaceae Salisbury
7. Dracaeneae Dumortier
Trees to rhizomatous/stoloniferous herbs; roots often orange, velamen +; (monocot secondary thickening +); vascular bundles amphivasal [?level]; vessels in stem 0; (resin +, red, from wounds); plant glabrous; leaves (amphistomatic), 2-ranked/spiral, often pseudopetiolate, (fleshy, terete); inflorescence racemose, (branched), (many-flowered clusters); (bracts 0), bracteoles 0 (+); T ± connate; A adnate to T tube; filaments (flattened/inflated); stigma capitate to 3-lobed; ovule 1/carpel; fruit baccate, endocarp persistent, sclerotised, enclosing seed; seeds [really drupelets] often 1-2; testa obsolete; endosperm bony, ?embryo; n = 19-21.
1/170. Largely Old World, a few species in Hawai'i, Cuba and Central America.
Synonymy: Dracaenaceae Salisbury, Sansevieraceae Nakai
7. Rusceae Dumortier
Shrubs to climbers; chrysophanol + [anthroquinone, in the roots]; roots with velamen, cuboidal styloids +; (vessels in stem 0); plant glabrous; leaves spiral, scarious, cladodes +; inflorescences axillary; flowers (imperfect): T free to connate; filaments connate, (T connate, A adnate to T); staminate flowers: A (?3), anthers extrorse; (pollen inaperturate); pistillode +; carpelate flowers: staminodes +; placentation axile to parietal; ovules 2/carpel or 1-4/ovary, hypostase +; fruit a berry; testa disintegrates, tegmen thick-walled, exotegmen cells longitudinally and endotegmen transversely elongated; endosperm thick-walled, hemicellulosic, embryo short to medium; n = 20.
3/8: Ruscus (6). Madeira and the Canary Islands to the Caspian Sea, scattered. Photograph: Ruscus flower.
Synonymy: Ruscaceae M. Roemer, nom. cons.
Evolution: Divergence & Distribution. Biogeographical relationships in the Dracaena group are of considerable interest. It has beeen suggested that Pleomele (= Chrysodracon) from Hawai'i is sister to the rest of Dracaeneae (e.g. Lu & Morden 2010, 2013, 2014), which raises all sorts of biogeographical questions such as, is Chrysodracon an old inhabitant of the islands, like Hillebrandia? (see also Price & Wagner 2018). In turn Central American species are sister to the remainder. However, Takawira-Nyenya et al. (2018) recently recovered a rather different set of relationships, for instance, Chrysodracon was embedded in Dracaena (the American species were not sampled), which suggest a rather different story. Lu and Morden (2014) also noted several independent transitions to the arborescent habit (perhaps four times) and the development of cylindrical leaves (ca seven times, all in the erstwhile Sansevieria).
Ecology & Physiology. Jura-Moraviec and Marcinkiewicz (2020) discuss water uptake and storage by the leaves of Dracaena draco.
Pollination Biology & Seed Dispersal. The flowers of Aspidistra (Convallarieae), sometimes borne beneath the litter, have a relatively huge, fungiform stigma, the anthers being hidden below it (Endress 1995b; Vislobokov 2017), and they show a considerable amount of variation. Flowers of some species look rather those of some Aristolochiaceae or Burmanniaceae, while others are more conventional and sub-rotate with the stamens and stigma/style grouped in the centre, or they have a short corona at the apex of the perianth tube that is massively longitudinally-ridged, or they have a balloon-like perianth with a little opening at the apex. There may be anything from two to a dozen or more tepal lobes (see also Hou et al. 2009; G.-Z. Li 2004; Vislobokov et al. 2014a; Vislobokov 2017). Easy access to the inside of the flower is apparently blocked, there is no nectar, rarely any appreciable (to humans) scent, no thermogenesis, and no distinctive UV colour patterning, at least in the few species examined (Vislobokov 2017). It has been suggested that such flowers are pollinated by amphipods (Conran & Bradbury 2007 and references, perhaps least likely), fungus gnats (Suetsugu & Sueyoshi 2017), the phorid fly Megaselia (Vislobokov et al. 2013), drosophilids, or bnon-galling cecidomyiid midges (Cecidomyiidae, undetermined genus) which also lay eggs in the anthers, the larvae eating the pollen (Vislobokov et al. 2014b; Vislobokov 2017). A remarkable and speciose genus in which new species are being described at quite a rate.
Vegetative Variation. Vegetative variation is particularly impressive. Dracaeana is the only monocot known with a monocot cambium in its roots as well as its stems (Carlquist 2012a; see also below). Thickening of the massive "trunk" of Dracaena draco, which can reach some 8 m d.b.h., is in substantial part by the fusion of massive aerial roots the cells of which, like those of the roots of orchids, etc., have chloroplasts, with the trunk proper (Krawczyszyn & Krawczyszyn 2014) - sort of corticating roots... The leaves of Dracaena draco have hypodermal bands of fibres and variously-oriented collateral bundles scattered through the blade (Jura-Moraviec & Marcinkiewicz 2020). Nolina also has secondary growth in the stem and is tree-like, and Beaucarnea, also tree-like, has a much swollen stem base. The initiation of the vascular system in the rhizome of Ophiopogon is similar to that in palm stems (Pizzolato 2009).
Eriospermum includes perhaps the most remarkable foliar variation of any genus of vascular plants. The leaf blades can have enations on the upper surface, and these include fungiform protrusions on the small, crisped, ovate and fleshy blade (E. titanopsoides), a much-branched structure to 12 x 7.5 cm on a much smaller blade (E. ramosum), a bundle of enations with stellate hairs (E. dregei), and paired enations that look as if they should grace the helmets of the Valkyries (E. alcicorne), while in E. aphyllon the plant when at the flowering stage appears to lack leaves, photosynthesis being carried out by the persistent inflorescence axis and pedicels (see Perry 1994 for more details). These may be adaptations for catching water from fog in the arid coastal regions of southwest Africa where they grow (Vogel & Müller-Doblies 2011).
Classical morphology suggests that the fleshy leaf of Sansevieria (= Dracaena) develops from the leaf base, the apical portion of the leaf being represented by a Vorlaüferspitze (e.g. Kaplan 1997, vol. 2: chap. 16); depending on the species, the leaf can be developed predominantly from the base (and is flattened) or from the apex (and is terete: Kaplan 1973).
Ruscus and its immediate relatives have cladodes, the flowers being born in the middle of a tough, more or less elliptical leaf-like structure. The prophylls are lateral or in some interpretations completely adnate to the axillary shoot, together they form an expanded cladode (Arber 1924a, 1930), or they are homeotic structures (Cooney-Sovetts & Sattler 1987). In any event, the leaves proper are small and scarious and subtend the cladodes (see also Asparagus above).
Genes & Genomes. See Yamashita and Tamura (2004) for chromosomes in Convallarieae and G.-Y. Wang et al. (2013) for those in Ophiopogoneae.
In Ruscus and immediate relatives a mitochondral cox2 intron is missing (Kudla et al. 2002).
Economic Importance. For the fabled dragon's blood, red resinous exudate produced after damage by some eleven or so not all immediately related species of Dracaena that are scattered from the Cape Verde islands to Vietnam, see Madera et al. (2020) and Durán et al. (2020). The species include D. draco, from Cape Verde islands, etc., and D. cinnabari, from Socotra. Dracaena draco may have (been) moved quite recently from the Canary Islands to Madeira and Morocco.
Chemistry, Morphology, etc.. Vanícková et al. (2019) analysed the resin of dragon's blood (Dracaena spp.), i.a. monoterpenes appeared to be species-specific. Although Madera et al. (2020) mention that Dracaena trees branch dichotomously, the inflorescences are terminal and branching is pseudodichotomous.
The absence of septal nectaries in some Nolinoideae may be connected with the presence of prominent ovary wall obturators; the latter are possibly derived from the former. In Liriope, etc. (Ophiopogoneae), the seeds, with their fleshy testa, are exposed early in development, so they are semi-gymnospermous.
Additional information can be found in Bos (1998: Dracaenaceae) and Madera et al. (2020: dragon trees), Conran and Tamura (1998: Convallariaceae), Bogler (1998: Nolinaceae), Duthie (1940), Dahlgren (in Dahlgren & Van Wyk 1988), Perry (1994) and van Jaarsveld and Eggli (2020a), all Eriospermum/Eriospermaceae, Yeo (1998), Judd et al. (2002), Judd (2003) and Eggli (2020b), all Ruscaceae in some sense, general, Rudall & Campbell (1999: floral morphology), van der Ham (1994: Peliosanthes distinctive) and L. Wang et al. (2017: Polygonatae s.l.), both pollen, Stenar (1934, 1953), Wunderlich (1950), Eunus (1950b), Björnstad (1970), A.-m. Lu (1985: Eriospermum), Ebert and Greilhuber (2006: references) and Song et al. (2018: Polygonatum), all embryology, and Tillich (1995: seed, etc.).
Phylogeny The placement of Eriospermum (for which, see Perry 1994) as sister to the rest of Nolinoideae has quite strong support (Seberg et el. 2012, but c.f. ML analyses, linking quite strongly with Asparagoideae!). It might be thought that it and and the very distinct Comospermum are likely to be sister to the rest of the subfamily since both have capsules and hairy seeds. Note that the hairs on the seeds of the two genera develop in different ways, etc., and the two seem to be unrelated (Rudall 1999); they do not come out close in studies such as that of Seberg et al. (2012). The poorly understood Peliosanthes may then be sister to the rest of the family (molecular data alone, e.g. Jang & Pfosser 2002). However, in several analyses it groups with Ophiopogoneae (e.g. Seberg et al. 2012; G.-Y. Wang et al. 2014; Floden & Schilling 2018: support strong). Relationships within other Nolinoideae are poorly resolved, although major clades largely correspond with tribes (see Conran & Tamura 1998). Convallarieae may be paraphyletic with Aspidistreae and Ruscus and relatives embedded (Yamashita & Tamura 2000: Eriospermum not included; Rudall et al. 2000b; Seberg et al. 2012). Convallaria was also included in Aspidistreae by Floden and Schilling (2018: support strong, Ruscus not sampled). For relationships of ex-Nolinaceae, -Dracaenaceae, etc., see also Bogler and Simpson (1996); Dracaeaneae may be sister to Ruscus and relatives.
Polygonateae. Meng et al. (2014) discussed relationships within/between Polygonatum and its relatives. This tribe probably does not include Maianthemum, which may be best placed with Ophiopogoneae (support weak), otherwise relationships are [Disporopsis [Polygonatum + Heteropolygonatum]] (Floden & Schilling 2018: plastid genomes). Within Dracaeneae, Lu and Morden (2010, 2013, 2014: chloroplast data) found that Dracaena and Pleomele alternated up a highly pectinate backbone of the tree (many of the branches had moderate support), Pleomele from Hawai'i (= Chrysodracon) was sister to all other Dracaeneae, and American taxa sister to the remainder; Sansevieria was deeply embedded and polyphyletic, S. sambirananensis being in a separate clade (but Baldwin & Webb 2016 recognize the genus). However, recently Takawira-Nyenya et al. (2018: chloroplast and nuclear trees rather different) recovered a rather different set of relationships. Although Sansevieria was still polyphyletic and embedded in Dracaena and Pleomele, so was Chrysodracon (floral differences = bird pollination syndrome), but unfortunately American species were not sampled. For relationships in Macaronesian taxa of Dracaena, see Durán et al. (2020). Nolineae. Rojas-Piña et al. (2014) evaluate relationships around Beaucarnea and Nolina; there are three morphologically distinctive clades of tree-like plants there, although support for the monophyly of Nolina is not strong.
Classification. The tribal classification above does not pretend to be exhaustive, and it is not certain that all the tribes are monophyletic.
Maianthemum includes Smilacina since the whole clade is well supported as being monophyletic (Kim & Lee 2007; Meng et al. 2008); a broad circumscription is also appropriate because there is little support for groupings within it. Takawira-Nyenya et al. (2018) found that just about no taxa in previous classifications of Dracaena were monophyletic.
Jessop (1976) suggested that Peliosanthes teta might be the only species in the genus, the ovary varying from superior to inferior. However, it is currently thought that Peliosanthes includes some 60 species or more, and with new species being described (e.g. Tanaka 2018).
Previous Relationships. There has been extensive confusion between Dracaena (Nolinoideae-Dracaeneae) and Cordyline (Lomandroideae-Cordylineae).