- Research article
- Open Access
Anatomy and RNA-Seq reveal important gene pathways regulating sex differentiation in a functionally Androdioecious tree, Tapiscia sinensis
BMC Plant Biology volume 19, Article number: 554 (2019)
Gametogenesis is a key step in the production of ovules or pollen in higher plants. The sex-determination aspects of gametogenesis have been well characterized in the model plant Arabidopsis. However, little is known about this process in androdioecious plants. Tapiscia sinensis Oliv. is a functionally androdioecious tree, with both male and hermaphroditic individuals. Hermaphroditic flowers (HFs) are female-fertile flowers that can produce functional pollen and set fruits. However, compared with male flowers (MFs), the pollen viability and number of pollen grains per flower are markedly reduced in HFs. MFs are female-sterile flowers that fail to set fruit and that eventually drop.
Compared with HF, a notable cause of MF female sterility in T. sinensis is when the early gynoecium meristem is disrupted. During the early stage of HF development (stage 6), the ring meristem begins to form as a ridge around the center of the flower. At this stage, the internal fourth-whorl organ is stem-like rather than carpelloid in MF.
A total of 52,945 unigenes were identified as transcribed in MF and HF. A number of differentially expressed genes (DEGs) and metabolic pathways were detected as involved in the development of the gynoecium, especially the ovule, carpel and style. At the early gynoecium development stage, DEGs were shown to function in the metabolic pathways regulating ethylene biosynthesis and signal transduction (upstream regulator), auxin, cytokinin transport and signalling, and sex determination (or flower meristem identity).
Pathways for the female sterility model were initially proposed to shed light on the molecular mechanisms of gynoecium development at early stages in T. sinensis.
Angiosperm plants exhibit a wide variety of breeding systems [1, 2]. Among them, hermaphroditism is thought to be the ancestral breeding system in angiosperms [3, 4], and dioecy appears to have evolved from hermaphroditism multiple times [1, 5,6,7]. Although two main pathways for the evolution of dioecy have been proposed, dioecy that evolves from an ancestral hermaphrodite or from a monoecious species is considered to be the most common [1, 6,7,8,9]. On this pathway, it is believed that hermaphroditic individuals coexist with unisexual mutants that have lost either their male (gynodioecy) or their female (androdioecy) function . Among the variety of reproductive mechanisms in flowering plants, one permutation – androdioecy (mixtures of males and hermaphrodites) – is distinguished by its rarity and represents less than 0.005% of all angiosperms . However, androdioecy is thought to be relatively unstable; models of mating system evolution predict that androdioecy should be a brief stage between hermaphroditism and dioecy (separate males and females), or vice versa [5, 8, 9, 11,12,13,14,15]. Loss of function is not a big challenge. The biggest challenge to female sterilty is due to natural selection. Typically if an individual looses female fertility, its fitness will be halved, and natural selection should act against it, eliminating the mutation.
Separate sexes have evolved on numerous independent occasions from hermaphroditic ancestors in flowering plants . Mechanisms controlling sex can be genetic, epigenetic (physiological and environmental) [17,18,19,20,21,22,23,24], or plant hormones [2, 25]: (1) Genetic control of sex determination is driven by chromosomes and sex determining genes in the dioecious plants. According to Heikrujam et al. (2015), genetic sex determination may be due to a single locus or multiple loci either unlinked or tightly linked on autosomes . For example, in persimmon, only a single locus is responsible for sex determination [26, 27] while the evolution of separate sexes in asparagus invokes sterility mutations at two linked loci [27, 28]. (2) Hormonal regulation of unisexual flower development . Unisexual flower development in Cucumis sativus (cucumber) and Cucumis melo (melon) is regulated by the interaction of environmental cues, plant hormones and genetic factors that differentiate gender phenotypes [24, 25, 30]. In kiwifruit, a Y-encoded suppressor of feminization, Shy Girl, arose via lineage-specific duplication of a cytokinin response regulator . At present, in some plant species, such as Arabidopsis [31, 32], cotton , rice , tomato , Silene latifolia [36, 37], Zea mays [38,39,40], Diospyros lotus , and cucumber , significant progress in elucidating the molecular mechanism of pistil development and sex determination has been achieved [24,25,26]. Molecular studies in these species have led to important advances in our understanding of plant sex determination and differentiation [25, 26, 41]. For example, ANT promotes ovule primordium growth; the CUP-SHAPED COTYLEDON genes (CUCs) play a role in the establishment of the ovule primordium boundaries; when the functions of stk, shp1, and shp2 were lost in a triple mutant, fewer ovules were initiated, and ovule development was severely disrupted. Even more remarkably, the ABCDE model of flower determination and development has indicated that a specific class of MADS-box genes are key regulators of pistil development , such as AGAMOUS (AG), APETALA 2 (AP2), BELL 1, INNER NO OUTER (INO), AINTEGUMENTA (ANT), SPOROCYTELESS (SPL/NZZ), and SUPERMAN (SUP) [43, 44].
Recent advances in the evolution of androdioecy showed that androdioecy arose from hermaphroditism because some male flowers have non-functional pistils, and that these residual organs are common in androdioecious and gynodioecious species that arose from hermaphroditism [13, 45,46,47,48,49], and that in species where androdioecy arose from dioecy, non-functional pistils are absent [50, 51]. In the functionally androdioecious Tapiscia sinensis Oliv. (Tapisciaceae) [52,53,54], the male individuals have pistillode, some of which have a shorter column and abortive ovule, while the vast majority of pistils lack ovaries (Figs. 1 and 2a). Thus, this plant might provide a perfect model of male individuals that originated from an ancestral hermaphrodite. Furthermore, the stage at which pistil abortion occurs and sex differentiation is determined by sex chromosomes, sex-determining genes, or hormone regulation remians unclear.
To determine the molecular mechanism of female sterility in male individuals, we compared the developmental anatomy and performed transcript profiling using the RNA-Seq technique of the gynoecia of the HF and MF. A number of candidate genes and related pathways were revealed, which provided new insights into the genetic and biochemical controls for early stages of pistil development, and our results will be helpful in shedding light on the mechanism of sex differentiation in the functionally androdioecious trees of Tapiscia.
The morphology of MFs is funnel-shaped, whereas that of HFs is water goblet-shaped (Fig. 2a) and have a normal pistil with a stigma, a style, and an ovary (Fig. 2c). In comparison with HF, the gynoecia of MF were slow-growing and much shorter from the early development stage to flowering (Fig. 2b, g). In natural populations, the MFs have three types (Fig. 2b, d-f). In comparison with Type III, the ovary transverse diameters (OTD) in Type I and Type II is smaller (p < 0.05) (Fig. 2i), while no significant differences exist among their pistil lengths (PL) (Fig. 2j). Correspondingly, the flowering duration of MF plants was prolonged until complete fertilization of HF because they had no seed setting and produced more flowers. MF had shorter pistils, and smaller ovules than HF. At flowering time, MF bloomed at a PL of 1.17 ± 0.17 mm (Fig. 2g) and an OTD of 0.518 ± 0.05 mm (Fig. 2h). In contrast, HF bloomed at a PL of 2.63 ± 0.54 mm (Fig. 2j) and an OTD of 1.15 ± 0.08 mm (Fig. 2i). The OTD (T = -7.102, df = 12, P < 0.01) and the PL (T = − 2.876, df = 12, P < 0.05) were clearly shorter in MF than in HF. Remarkably, in MFs, the PL and OTD remain unchanged when the bud vertical diameter grew to 0.75 ± 0.05 mm (stage 9, May 16th) (Fig. 2d). Later, some limited growth may continue from stage 9 to flowering for the carpel in MFs, which is often only one-quarter to one-half the full length that in the HFs (Fig. 3j).
The SEM results showed that there were no obvious differences observed between MF and HF before stage 5 (Fig. 3a). However, at stage 6, in HFs, the gynoecium primordial begins to form as a ridge of raised cells around the center of the flower apex (Fig. 3a, b, c). At stage 7, the gynoecium grows as a hollow tube (Fig. 3c, d); At stage 8, the gynoecium tube grows taller and wider, the gynoecium continues to grow upward to form a continuous hollow cylinder, and placenta primordia were observable; during stage 10, in the centre of the receptacle, ovule primordium were observable (Fig. 3e, f); at the flowering time (stages 11–14), the gynoecium becomes ready for fertilization, and when the stamens extend out of the petal, fertilization occurs (Fig. 3g, h).
In most MFs, during stage 6, the gynoecium primordium began to form (Fig. 3b), but the central zone was fused as a hemispherical bulge and no differentiation of the ring meristem is present (Fig. 3c, d), which was obviously different from the ring meristem in HFs (Fig. 3b, c). The pistil structure of the MF was characterized by the formation of a solid, stem-like structure (Fig. 3e-g). The key stage at which ovule abortion occurred was stage 6 (Fig. 3b, B).
Structure of the flower
In T. sinensis, the course of individual flower development can be divided into five phases: early differentiation, calyx initiation, petal initiation, stamen initiation, and carpel initiation. The perianth was the first organ to be formed on the floral apex (Fig. 4a, b). Sepals differentiated concurrently and curved to cover the central zone (Figs. 3a and 4c). In late stage 5, petal and stamen primordia are initiated (Fig. 4d). As the stamens formed, there was a bud vertical diameter of 76.92 ± 1.98 μm, and the floral apex became broadly concave (Fig. 4e). The central zone (floral meristem) of the flower bulges out to form a platform on which the gynoecium primordia will develop (Figs. 4f, g and 3b). At stage 6, the sepals enclose the flower bud, and two or three carpel primordia begin to form, with raised cells around the floral apex constituting a ridge (ring meristem) (Fig. 4h, i). At stage 7, the medial stamens become stalked at their bases, and the ring meristem grows as a hollow tube (vertical section) (Fig. 4j~l); at stage 8, the placenta primordium is observable (Fig. 4m~o); then, the ovule forms from the placenta (Fig. 4p, q). The two or three carpels gradually fused with each other in hermaphrodites and eventually developed into a normal pistil with a stigma, a style, and an ovary (Additional file 4: Figure S1).
From stage 1 to stage 5, hermaphroditic individuals and males have the same developmental process and morphological structures (Fig. 4a-k). However, after stage 5, the carpel primordium of the centre of the floral apex in MFs exhibits different patterns from that of HFs. Longitudinal sections of MF from the same tree showed that there are three types of pistils. Type I: Most of the MFs without ovules or ovaries were characterized by the formation of a solid, stem-like residual pistil (Fig. 5a-i). Type II: A tiny minority (1.6%) of MF had one ovary but no ovule structure (Fig. 5j-n). Type III: MFs have a well-developed pistil that is sterile (3.33%); the ovary has one chamber that has one ovule that has double integuments and is crassinucellate and anatropous (Fig. 5o-u); however, when the MF falls off after maturation, termination of embryo sac development occurs at the triad stage (Fig. 5v; Additional file 4: Figure S1).
A pollination analysis found that a few pollen grains from self or HF could germinate on MF stigmas 6 h after pollination. Remarkably, compared with HF (Fig. 6a-c), in MF, although pollen tubes could grow in a spiral manner over the surface of the papilla cells, some of them penetrated into stigmas or styles and then succeeded in reaching the abnormal ovules 24 h after pollination (Fig. 6a-c). Further observation showed that the papilla cells on MF stigmas (Fig. 6d, e) were similar to HFs at the maturation stage (Fig. 6d, e). The anther and pollen grain sections show that many sterile pollen grains (spg) were observed in HF (Fig. 6f) but not in MF (Fig. 6f). There are two types of pollen in hermaphroditic flowers (Fig. 6g), while there is only one type of pollen in MF (Fig. 6g). In contrast to the perforate tectum of the olivary pollen grains in MF (Fig. 6h, i), the pollen grains in HF have a reticulate tectum (Fig. 6h, i).
Illumina sequencing and sequence assembly
In this project, the Illumina HiSeq™ 4000 sequencing platform was used for transcriptome sequencing, and 962,641,935 clean reads were obtained, with a mean length of 150 base pairs (bp). The average GC percentage was 44.69%. The clean reads were de novo assembled using Trinity  into 63,573 contigs, with a mean length of 1132 bp and an N50 of 1892 bp. Then contigs were used for sequence clustering with the software TGICL (TIGR Gene Indices clustering tools) to form unigenes . The total number of unigenes was 52,945, with a mean length of 973 bp and N50 of 1768 bp. The average depth of sequence coverage was 82.42%. In all, 36,353 unigenes within 201–1000 bp, which was 57.59% percent. Additionally, 7766 unigenes (14.67%) ranged from 1001 to 2000 bp in length, while 7408 of the unigenes (13.99%) were over 2000 bp in length.
Differentially expressed genes (DEGs) and enrichment analysis
Using the series test of cluster (STC) , a total of 9989 and 7326 unigenes were identified and transcribed in the M1-M2-M3 term (TERM1)_vs_H1-H2-H3 term (TERM2), respectively (Additional file 4: Figure S3). M1, M2 and M3 represent MF at stages 5, 6 and 10, respectively, while H1, H2 and H3 represent bisexual flowers at stages 5, 6 and 10, respectively. In TERM1, the expression patterns of 13,761 genes were analysed, and eight model profiles were used to summarize (Additional file 4: Figure S2); five expression patterns of genes showed significant p-values (p < 0.05) marked with coloured boxes, including profile 3, profile 4, profile 5, profile 6, and profile 7 (Additional file 4: Figure S3). In TERM2, the expression patterns of 16,130 genes were analysed, and eight model profiles were used to summarize (Additional file 4: Figure S2); three expression patterns of genes showed significant p-values (p < 0.05) marked with coloured boxes, including profile 1, profile 6, and profile 7 (Additional file 4: Figure S3). Each box represents a model expression profile with the model profile number and p-value. To further clarify the functional differences between MF and HF at stage 6, using a false discovery rate (FDR) ≤ 0.05 and the absolute value of |log2 ratio| ≥ 1 as criteria, 9623, 14,347 and 12,049 unigenes exhibited significantly different expression levels in M1_vs_ H1, M2 _vs_H2, and M3_vs_H3, respectively (Additional file 4: Figure S4A-C).
To determine whether the DEGs between MF and HF are significantly related to specific pathways or biological function, GO and KEGG databases were used for enrichment analysis (Additional file 4: Figure S4D-F). For TERM1, TERM2, M1_vs_H1 DEGs, the GO terms that showed enrichment included “flavonoid biosynthetic process” (GO:0009813), “secondary metabolic process” (GO:0019748), “hormone biosynthetic process” (GO:0042446), “cytokinin biosynthetic process” (GO:0009691), “glycoside biosynthetic process” (GO:0016138), and “regulation of fertilization” (GO:0080154) (Additional file 3). In contrast, for TERM1, TERM2, M2_vs_H2, the enriched classification terms were “cell wall organization or biogenesis” (GO:0071554), “external encapsulating structure organization” (GO:0045229), “glucose metabolic process” (GO:0006006), “embryo development” (GO:0009790), “response to inorganic substance” (GO:0010035), and “response to chemical” (GO:0042221) (Additional file 3).
Pathway assignment was carried out by KEGG to analyse the biological functions of DEGs. For the TERM1, TERM2, and M1_vs_H1 comparison (Fig. 7a), pathways related to “Phenylpropanoid biosynthesis” (ko00940), “Plant-pathogen interaction” (ko04626), “Plant hormone signal transduction” (ko04075), “Glucosinolate biosynthesis” (ko00966), “Diterpenoid biosynthesis” (ko00904), “Starch and sucrose metabolism” (ko00500), “Zeatin biosynthesis” (ko00908), “Ribosome” (ko03010), and “Flavonoid biosynthesis” (ko00941) were enriched (Additional file 3). For the TERM1, TERM2, and M1_vs_H1 comparison (Fig. 7b), the main pathways included “Glycolysis/Gluconeogenesis” (ko00010), “Pentose and glucuronate interconversions” (ko00040), and “Tryptophan metabolism” (ko00380), “Citrate cycle (TCA cycle)” (ko00020), “Starch and sucrose metabolism” (ko00500), “Plant hormone signal transduction” (ko04075), and “Zeatin biosynthesis” (ko00908) (Additional file 3). The enrichment analysis revealed a total of 63 DEGs related to plant hormone signal transduction. Thus, the process of “plant hormone signal transduction” was concluded to be a putative pathway affecting T. sinensis flower development (Additional file 3).
In brief, the DEGs were characterized using the GO and KEGG databases. Based on recent research results [25, 29, 31, 42, 44], we will focus on gene regulatory network models related to carpel and ovule development, “Plant hormone signal transduction” (ko04075), “Zeatin biosynthesis” (ko00908), “hormone biosynthetic process” (GO:0042446), and “cytokinin biosynthetic process” (GO:0009691) (Additional files 2).
Gene regulatory network (GRN) models related to carpel and ovule development
The results of scanning electron microscopy (SEM) and light microscopy (LM) show that most of the vestigial pistils of MF of T. sinensis developed into finger-like structures without ovary or ovule. Pollen germination and pollen tube growth in MF indicated that pollen tubes can grow in the stigma/style and that they are functional, and therefore, ovules are never present is the main factor responsible for female-sterility of male flowers (Fig. 8a). In Arabidopsis, ovule cell fate is controlled by ovule identity genes [31, 44, 58,59,60]. The pathway of regulation of Arabidopsis ovule development is shown in Fig. 7, and key regulators include AG [30, 61, 62], SPL , INO , ANT and BEL1 [31, 65]. Carpels are the most complex structures within flowers; a GRN (gene regulatory network model) underlies their development in Arabidopsis , and in T. sinensis, the key regulators were identified, including WUS (Unigene0010686), AGAMOUS (Unigene0020941), SUP (Uniene0047137), SPL (Unigene0006964), INO (Unigene0025624), STM (Unigene16944), ANT1 (Unigene0002499), STK (AGL11) (Unigene0007536), SHP1 (Unigene0013614), AP2 (Unigene0015664), TSO1 (Ungene0002282), SPT (Unigene0034455), LUG (Unigene0041412), PI (Unigene0020391), SEUSS (Unigene0033961) and BEL1 (Unigene0039261) (Fig. 8b, c). In the MF-HF comparison, these 16 genes showed significantly different expression levels. The results indicated that these genes may influence the flower development.
To confirm that the unique-match genes from the Illumina sequencing and bioinformatics analysis were indeed differentially expressed, a total of 16 genes were selected from the DEGs related to flower development (including carpel, ovule, pollen) for quantitative RT-PCR assays. For 16 genes, the qRT-PCR analysis revealed the same expression trends as the RNA-Seq data, despite some quantitative differences. All genes had different expression levels between MF and HF at stage 6 (Fig. 8d). For example, at stage 6, Unigene0020941, a transcription factor that regulated carpel development, was down-regulated (0.018 to 0.045) in MF relative to HF by qRT-PCR, the same trend as the one (39 to 338) from RNA-Seq.
Identification of genes involved in ethylene biosynthesis and signal transduction
Ethylene regulates many aspects of plant development and responses to biotic and abiotic stress. We identified ten DEGs involved in the ethylene biosynthesis and signal transduction process (Fig. 9a): ACO (Unigene0029908), ACO1 (Unigene0037768), ACS (Unigene0021193), ERS1 (Unigene0024060), CTR1 (Unigene0036282), TIR1 (Unigene0037222), ETR1/2 (Unigene0020715, Unigene0027393), EIN2/3/4 (Unigene0029458, Unigene0050718, Unigene0003076) (Fig. 9b). To confirm the results of RNA sequencing, ten DEGs related to carpel development were selected for qRT-PCR analysis (Fig. 9c). The results showed similar expression trends to the transcriptome analysis, and only 2/16 genes (EIN2 and EIN3) had different results in qRT-PCR vs RNA-Seq, confirming the reliability of the RNA-Seq data. 1-aminocyclopropane-1-carboxylic acid (ACC) synthase (ACS) is the rate-limiting enzyme in ethylene synthesis, and it is important in regulating ethylene biosynthesis. Unigene0021193 was downregulated at stage 6 in the M-H comparison. Two ACC oxidase homologous genes showed different expression patterns, but ACO and ACO1 were both upregulated in stage 6 in the MF-HF comparison.
In Arabidopsis, the perception of ethylene is achieved by five members of a family of ER membrane-bound receptors: ETR1, ETR2, ERS1, ERS2 and EIN4, some of which have histidine kinase activity . From mRNA sequencing, we obtained four ethylene receptors: EIN4 (Unigene0003076), ETR2 (Unigene0027393), ETR1 (Unigene0020715), ERS1 (Unigene0024060). At stage 6, the relative expression of Unigene0020715 displayed significant differences, but Unigene0027393 and Unigene0024060 were indistinctive. Unigene0020715, the repressor of ethylene signal transduction, was up-regulated in MF relative to HF, but Unigene0027393 displayed indistinctive expression. Similarly, Unigene0003076 displayed almost the same trend as ETR1 during stage 6, while Unigene0024060 was indistinctive. ERF1/2 (Unigene0025860, Unigene0005688), the downstream gene in the ethylene signal transduction pathway, displayed differential expression in both the M1-M2 and H1-H2 comparisons, being up-regulated in MF relative to HF at the key stage. Obviously, at stage 6, ACO (Unigene0029908), ACO1 (Unigene0037768), CTR1 (Unigene0036282), and EIN2 (Unigene0029458) were up-regulated in the MF-HF comparison, while ACS and EIN3 were down-regulated in MF relative to HF.
To verify the role of ethylene in sex differentiation of T. sisensis, we sprayed ethephon at concentrations of 150 mg/L. We found that ethephon had a significant effect on MF transformed into HF.
Identification of genes involved in Auxin and Cytokinin signal transduction
The third related pathway was the auxin transport and signalling pathway. As the first plant hormone studied, auxin has wide-ranging effects on growth and development throughout the plant, including gynoecium and ovule morphogenesis [73,74,75]. In our study, we identified 24 DEGs involved in auxin and cytokinin signal transduction (Fig. 10a, b): IAA31 (Unigene0018133), IAA26 (Unigene0035359), IAA15 (Unigene0001116), IAA19 (Unigene0025767), GH3.1 (Unigene0015426), SAUR2 (Unigene0017779), SAUR14 (Unigene0050945), SAUR72 (Unigene0005319), SAUR50 (Unigene0010084), SAUR12 (Unigene0018267), SAUR31 (Unigene0049968), SAUR53 (Unigene0019490), KUP3 (Unigene0005158), MIR397B (Unigene0025946), ARR10 (Unigene0049560), AHP4 (Unigene0004154), AHP6 (Unigene0011561), AHP4 (Unigene0004325), IAA1 (Unigene0001116), ARF17 (Unigene0029174), CALS5 (Unigene0019058), PIN6 (Unigene0020253), PIN2 (Unigene0033811), PIN1 (Unigene0000533). To confirm that the unique-match genes from the Illumina sequencing and bioinformatics analysis were indeed differentially expressed, a total of 9 genes were selected from the DEGs related to flower development for quantitative RT-PCR assays. Among 9 of the 24 genes with different expression levels between MF and HF (Fig. 10c) at stage 6, six genes were up-regulated in MF relative to HF, and three genes were down-regulated.
The male flowers of T. sinensis originated from ancestral hermaphroditic flowers
A variety of hypothesized evolutionary pathways have been proposed for the evolution of dioecy from hermaphroditism, and the production of only bisexual flowers is the ancestral condition in angiosperms [3, 7, 16, 78,79,80,81,82,83]. Theory predicts that at least two mutations are necessary to evolve separate sexes . One must result in male sterility while the second must result in female sterility [27, 29]. Therefore, we examined whether the androdioecy of T. sinensis resulted from transformation from female flowers to restore male function in dioecious plants or was caused by pistil sterility in bisexual flowers.
In T. sinensis, male flowers in each natural population possess the characteristic of a vestigial pistil, and the receptive stigma is covered by papillary cells. Although the degree of sterility of pistils is different, the males have the potential to form ovules. In addition, in natural populations, no pollen limitation on the reproduction of T. sinensis [84, 85]. Therefore, female flowers evolved from female flowers are unlikely to restore their male function to ensure reproduction . Obviously, it is also unreasonable for MF to evolve a pistil if androdioecy arose from dioecy. In addition, as in Osmanthus fragrans L., the MF has a vestigial pistil, also suggesting that males evolved from female-sterile mutants among hermaphrodites .
The breeding system and other traits mapped on the phylogenetic tree of Fraxinus L. (Oleaceae) show that dioecy has three separate origins; in one instance, dioecy evolved from hermaphroditism via androdioecy following the transition from insect to wind pollination [45, 86]. Dioecy may also evolve in conjunction with the evolution of wind pollination in some previously insect-pollinated species [87, 88]. T. sinensis is a wind-pollinated and insect-pollinated species [52, 53], and this mixed pollination pattern may be a possible evolutionary pathway from hermaphroditism to dioecy . A trend in tectum sculpture character state change from perforate to reticulate appears to be common in angiosperms [66, 67, 89]. In T. sinensis, the tectum sculpture is reticulate in MF pollen grains, while that of HF is perforate. Additionally, globose pollen grains have the largest volume-to-surface area ratio, but with minimal regulatory function, which is a relatively primitive character . Olive pollen grains can be transformed from the globose pollen grains of HF. Evolutionarily, this result also implied that hermaphroditism is more ancestral .
Key regulatory factors of pistil development may be associated with T. sinensis sex differentiation
Admittedly, ovule primordia arise from the placenta; however, both ovules and placenta are completely absent in most MFs of T. sinensis. Transcriptome analyses showed that sixteen genes related to carpel and ovule development are expressed differentially at the key stage of MF pistil abortion and were verified by qRT-PCR. The molecular mechanisms of ovule development in Arabidopsis, cotton, and rice are relatively well known [24,25,26, 90]. The C-class gene AG (AGAMOUS) belongs to the MADS-box family, which determines stamen and carpel identity and plays a role in ovule development [31, 44]. The SHP1 (SHATTERPROOF 1), SHP2 (SHATTERPROOF 2), and STK (SEEDSTICK) genes together with the SEP (SEPALLATA) genes have overlapping expression patterns with AG in an AG-independent manner . ANT (AINTEGUMENTA), HLL (HUELLENLOS), SIN2 (SHORT INTEGUMENT 2), INNER NO OUTER (INO), and SUPERMAN (SUP) as regulators of ovule outgrowth [31, 76, 90, 91]. AG is necessary for the determination and termination of floral meristem activity. In the ag mutant, delayed floral meristem activity results in the stamens and carpels being replaced by flowers . WUSCHEL (WUS), which specifies stem cell identity, and AG play crucial roles in regulating the initiation or termination of floral meristems [92, 93].
Previous studies have indicated that SPL/NOZZLE is required for the initiation of sporogenesis and plays a central role in nucellus formation by antagonizing the expression of BELL, ANT and INNER NO OUTER . Here, four genes are shown to be differentially expressed in MF relative to HF at stage 6. Moreover, SPL represses the expression of ANT and INO to control ovule primordium formation . SPL was downregulated in the key stage of pistil abortion in MF relative to HF, which indicated the role of SPL in promoting ovule development. However, during ovule development, BEL1 and SPL are required for cytokinin and auxin signalling for the correct patterning of the ovule .
In addition, the STM gene is considered to play a pivotal role in sustaining stem cell function in the floral apical meristem (STM is required for maintenance of WUS expression but independent of WUS expression) and controls KNOX gene expression independently of the transcriptional repressor AS1 [97, 98]. More precisely, STM plays a crucial role in preventing meristem cell differentiation by inducing the production of cytokinins (CK) and the ARR transduction pathway . The progressive loss of STM causes floral phenotypes ranging from reduced formation of placental tissues and inhibited carpel fusion to complete loss of carpel development . In T. sinensis, STM also showed differential expression, which indicated the role of STM in promoting ovule development.
In Arabidopsis, the ovule primordia arise from the placentas flanking the medial ridges, while leunig (lug) aintegumenta (ant) double mutants lack medial tissues, and the double mutant seu-3 ant-1 results in a complete loss of ovule initiation, caused by severe defects in early gynoecium development . CRABS CLAW (CRC) is a member of the YABBY gene family, whose expression is largely limited to carpels and nectaries, and plants expressing 35SCaMV::CRC produce variable flowers with partial transformations of sepals into carpels and reductions in flower organ number. Carpels are short and solid (ovule is completely absent) and composed primarily of stylar tissues. The morphology of the pistillode of MF in T. sinensis was similar to that of the Arabidopsis 35SCaMV::CRC pistil .
Ethylene may act as an upstream factor for female sterility in male flowers
The ETR1 protein acts as negative regulator of ethylene responses , has the function of promoting cell elongation. In T. sinensis, ETR1 (Unigene0020715) was up-regulated in MF relative to HF. ERF1 and ERF2, as ethylene response signal factors, were differentially expressed between MF and HF. The down-regulation of ERF1/2 and up-regulation of ETR1 may be related to the flower development. ACO and ACS (ACS and ACO are rate-limiting enzyme) are a pivotal enzyme in ethylene biosynthesis, they are showed significant expression levels in pistil formation ant stage 6. Jointly, our findings indicated that ethylene may act as one of the upstream regulators influencing the development of pistil. Furthermore, ANT, an APETALAP2-like Gene, plays fundamental roles in ovule formation and megasporogenesis [38, 104, 105], the down-regulation of ANT may be responded to ethylene. However, the expression of ANT and INO (INNER NO OUTER) may be regulated by AG and SPL.
Auxin and Cytokinin are required for ovule Primordia formation
Auxin maxima are fundamental for the formation of primordia, and auxin action has been well described for lateral roots and primordial flowers [44, 106, 107]. The directionality of the auxin flux depends principally on the polar localization of the PIN proteins. In Arabidopsis, there are eight PIN proteins (PIN1–8), from which only PIN1 and PIN3 are expressed in the pistil and ovules. For example, polar auxin transport is mostly mediated by the PINFORMED1 (PIN1) efflux carriers . Based on the phenotypes of pin mutant, gynoecia display a range of phenotypes from almost normal structures with two valves, style and stigma, to stalk-like gynoecia with an elongated gynophore topped with a style and stigma . The protein kinase PINOID (PID) positively regulates auxin efflux, which can control an early general step in meristem development. In the pid-l flower, the internal fourth whorl organ is stem-like rather than carpelloid, although it is capped with a ring of stigmatic papillae. Furthermore, the morphology of the vestigial pistil of MF T. sinensis was similar to that of the Arabidopsis pid-l pistil . Similarly, PINOID is required for formation of the stigma and style in rice . In addition, the crosstalk between CK and auxin plays a pivotal role in the boundaries in the inflorescence meristem and ovule primordia formation . Simultaneously, the Arabidopsis Histidine Phosphotransfer Protein 6 (AHP6), an inhibitor, mediates an auxin-cytokinin crosstalk that regulates the timing of organ initiation at the shoot apical meristem. In this study, genes that were expressed differently in MF relative to HF also supported this point.
In total, 29,585 out of 52,945 unigenes were annotated, and the KEGG enrichment analysis will provide valuable information on the sex differentiation of T. sinensis. First, ethylene is an upstream factor in T. sinensis gynoecium development, and signal transduction of auxin and cytokinin is fundamental to the initiation of pistil primordia; MADS-box genes were also shown to be involved in the determination of the fourth-whorl flower organs. In addition, auxin signalling pathways were thought to be involved in pollen abortion (partial pollen abortion in T. sinensis HF populations; Fig. 5) and were important for megagametophyte development (male mutant-Type III in MF; Fig. 1). Overall, a valuable new model of sex differentiation in T. sinensis was summarized, and further study of the functions of sex-related genes will be helpful in elucidating the sex-determination mechanism of the androdioecious plant T. sinensis (Fig. 11).
Flower sample collection
T. sinensis in natural populations has 2 sexual types: male individuals (MF, male flower) and hermaphroditic individuals (HF, hermaphroditic flower) with winter fruits. Two types of flowers of T. sinensis were sampled from the natural geographical distribution in Shennongjia National Nature Reserve (31°38′N, 110°25′E; Hubei, China) and the voucher specimens were deposited archived in the herbarium of Structural Botany Laboratory (SBL), Northwest University. Prof. Liu Wenzhe undertook the formal identification of the samples. Different growth stages of flowers were collected for our study. The flowers used for microscopic observation were fixed immediately in 2.5% glutaraldehyde, and those used for transcriptome analysis were stored in liquid nitrogen (LN) at − 80 °C.
A total of 18 samples were sequenced, comprising males and hermaphrodites in three different development stages (with three biological replicates for each stage). To describe the samples clearly, we used M1, M2, and M3 to represent MF buds when their development was at stage 5, stage 6, and stage 8, respectively (Fig. 1a-e). Stages are numbered as described by Sanders et al. (1999) . Three stages of samples were collected mainly according to the results of anatomy (Figs. 3d, e and 4); these stages represent the key stages that implied the formation of sexual dimorphism in T. sinensis. Similarly, H1, H2, and H3 represented the HF buds when their development was at stage 5, stage 6, and stage 8, respectively. Photographs are included showing the general developmental stages of the flowers (Fig. 1a-e).
RNA sequencing library construction, Illumina sequencing, and data processing
Total RNA (40 μg) was isolated from the M1, M2, M3 and H1, H2, and H3 samples using the TRIzol Kit (Promega, Beijing, China) and treated with RNase-free DNase (Takara Biotech Incorporation, Otsu, Japan). RNA quantity and purity were assessed using a Nanodrop 1000 spectrophotometer (Thermo Scientific, Waltham, MA, USA). RNA integrity (> 8.0) was determined using a Bioanalyzer 2100 (Agilent) with an RNA 6000 Nanochip (Agilent). Methods of enrich Mrna, remove rRNA, RNA fragment, random haxamer primed cDNA synthesis, size selection and PCR amplification were performed as previously described [43, 112, 113], and sequenced using Illumina HiSeqTM 4000 (Gene Denovo Biotechnology Co., Guangzhou, China).
De novo assembly and functional annotation
Raw data were processed with Perl scripts to ensure the quality of the data used in further analyses. The adopted filtering criteria are as Zhang et al. (2018) [55, 114]. The obtained clean data after filtering were used for statistical analyses of quality, including Q30, data quantity and quality, and base content statistics. The software Trinity-v2.6.5 was used for de novo assembly . TransDecoder identifies candidate coding regions within transcript sequences, such as those generated by de novo RNA-Seq transcripts assembled by Trinity. Functional annotation of transcript assemblies was performed using the included Trinotate pipeline (http://trinotate.sourceforge.net/) to identify open reading frames and assign best hits to UniProtKB (1e-03), PFAM-A (1e-03), Gene Ontology (GO) and eggNOG categories.
Screening of differentially expressed genes
To identify DEGs across samples or groups, the edgeR package (http://www.r-project.org/) was used. We identified genes with greater than a two-fold change and a false discovery rate (FDR) < 0.05 in a comparison as significant DEGs. DEGs were then subjected to an enrichment analysis of GO functions and KEGG pathways. Read count for each gene in each sample was determined by HTSeq (v0.6.0; http://www-huber.embl.de/users/anders/HTSeq/doc/overview.html), and RPKM (reads per kilobase per million mapped reads) was then calculated to estimate the expression level of the genes in each sample . The RPKM method is able to eliminate the influence of different gene lengths and sequencing data amounts on the calculation of gene expression. Therefore, the calculated gene expression can be directly used for comparing differences in gene expression among samples.
Differential expression analysis of the three stages in MF and HF was performed using DESeq . DESeq2 v1.4.5 was used for differential gene expression analysis, and a p-value could be assigned to each gene and adjusted by Benjamini and Hochberg’s approach for controlling the false discovery rate. Genes with q ≤ 0.05 and |log2_ratio| ≥ 1 were identified as DEGs. Gene expression patterns in all samples were compared with expression profiles for known Arabidopsis, Zea and Oryza carpel development or sex-determination genes [31, 58,59,60, 70, 78, 106, 115].
GO and pathway enrichment analysis of DEGs
The GO (Gene Ontology; http://geneontology.org/) enrichment of DEGs was implemented by the hypergeometric test, in which a p-value is calculated and adjusted as the q-value, and the data background is genes in the whole genome. GO terms with q < 0.05 were considered to be significantly enriched. GO enrichment analysis could reveal the biological functions of the DEGs , and we focused on genes that play roles in certain biological functions, i.e., those for which pathway enrichment analysis (KEGG, Kyoto Encyclopedia of Genes and Genomes) was mainly concerned with metabolic pathways or signal transduction pathways. Pathway analyses were performed with the KEGG pathway database using BLASTx with an E-value < 1 e-5 . The calculating formula is the same as that in GO analysis.
Here N is the number of all genes that with KEGG annotation, n is the number of DEGs in N, M is the number of all genes annotated to specific pathways, and m is number of DEGs in M. The calculated p-value was gone through FDR Correction, taking FDR ≤ 0.05 as a threshold. Pathways meeting this condition were defined as significantly enriched pathways in DEGs.
Real-time RT-PCR analysis
qRT-PCR was performed not only to analyze the expression levels of DEGs but also to verify the RNA-Seq analysis, which included ten genes (CTR1, ACS, ACO, ACO1, ETR1/2, ERS1, EIN2/3/4) related to ethylene biosynthesis and signal transduction, nine genes involved in auxin and cytokinin signal transduction, and sixteen genes related to carpel and ovule formation. Primer sequences were designed using Primer premier 5.0, and Primer sequences and β - actin (as an internal control to normalize the expression levels of genes) sequence of internal reference gene are listed in Additional file 1. RNA was extracted from T. sinensis of three developmental stages, and RNA extraction, cDNA synthesis, and Real-time PCR method as described in related references [116, 123].
Availability of data and materials
The datasets used and/or analyzed during the current study has been included within supplemental data. The plant materials are available from the corresponding author on reasonable request.
- ACO :
- ACS :
1-AMINOCYCLOPROPANE-1-CARBOXYLIC ACID SYNTHASE
- AG :
- AHP4/6 :
HPT PHOSPHOTRANSMITTER 4/6
- ANT :
- AP :
- BEL1 :
- CTR1 :
COPPER TRANSPORT PROTEIN 1
- CUC1/2 :
CUP-SHAPED COTYLEDON 1/2
differentially expressed genes
- EIN2/3/4 :
ETHYLENE INSENSITIVE PROTEIN 2/3/4
- ERS1 :
ETHYLENE RESPONSE SENSOR 1
- ETR1/2 :
ETHYLENE RECEPTOR 1/2
- IAA :
- INO :
NNER NO OUTER
- KUP3/50/72 :
K+ UPTAKE TRANSPORTER 3/50/72
- LUG :
ovary transverse diameters
- PI :
- PIN :
- PIN1 :
- SAUR :
SMALL AUXIN UPREGULATED
scanning electron microscope
- SEU :
- SHP1/2 :
- SPL/NZZ :
- SPT :
- STK :
- STY1 :
- SUP :
- WUS :
Vernet P, Lepercq P, Billiard S, et al. Evidence for the long-term maintenance of a rare self-incompatibility system in Oleaceae. New Phytol. 2016;210(4):1408–17.
Heikrujam M, Sharma K, Prasad M, et al. Review on different mechanisms of sex determination and sex-linked molecular markers in dioecious crops: a current update. Euphytica. 2015;201(2):161–94.
Endress PK. The flowers in extant basal angiosperms and inferences on ancestral flowers. Int J Plant Sci. 2001;162:1111–40.
Endress PK. Angiosperm ovules: diversity, development, evolution. Ann Bot. 2011;107(9):1465–89.
Vassiliadis C, Saumitou-Laprade P, Lepart J, Viard F. High male reproductive success of hermaphrodites in the androdioecious Phillyrea angustifolia. Evolution. 2002;56(7):1362–73.
Renner S, Won H. Repeated evolution of dioecy from monoecy in Siparunaceae (Laurales). Syst Biol. 2001;50:700–12.
Torices R, Mendez M, Gomez JM. Where do monomorphic sexual systems fit in the evolution of dioecy? Insights from the largest family of angiosperms. New Phytol. 2011;190:234–48.
Charlesworth B, Charlesworth D. A model for the evolution of dioecy and gynodioecy. Am Nat. 1978;112(988):975–97.
Lloyd DG. The maintenance of gynodioecy and androdioecy in angiosperms. Genetica. 1975;45(3):325–39.
Bradley D, Carpenter R, Copsey L, et al. Control of inflorescence architecture in antirrhinum. Nature. 1996;379(6568):791–7.
Akimoto J, Fukuhara T, Kikuzawa K. Sex ratios and genetic variation in a functionally androdioecious species, Schizopepon bryoniaefolius (Cucurbitaceae). Am J Bot. 1999;86:880–6.
Fleming TH, Maurice S, Hamrick JL. Geographic variation in the breeding system and the evolutionary stability of trioecy in Pachycereus pringlei (Cactaceae). Evol Ecol. 1998;12(3):279–89.
Xu YC, Zhou LH, Hu SQ, et al. The differentiation and development of pistils of hermaphrodites and pistillodes of males in androdioecious Osmanthus fragrans L. and implications for the evolution to androdioecy. Plant Syst Evol. 2014;300(5):843–9.
Charlesworth D. Androdioecy and the evolution of dioecy. Bot J Linn Soc. 1984;22:333–48.
Pannell JR. The evolution and maintenance of androdioecy. Annu Rev Ecol Syst. 2002;33(1):397–425.
Russell JRW, Pannell JR. Sex determination in dioecious Mercurialis annua and its close diploid and polyploid relatives. Heredity. 2015;114(3):262–71.
Wolf DE, Takebayashi N. Pollen limitation and the evolution of androdioecy from dioecy. Am Nat. 2004;163(1):122–37.
Kong DM. Progress in hormonal regulation to sex differentiation in higher plants. J Anhui Agric Sci. 2009;37(12):5352 -5354, 5378.
Irish EE, Nelson T. Sex determination in monoecious and dioecious plants. Plant Cell. 1989;1(8):737–44.
Khryanin VN. Role of phytohormones in sex differentiation in plants. Russ J Plant Physl. 2002;49(4):545–51.
Thomas TD. In vitro, modification of sex expression in mulberry (Morus alba) by ethrel and silver nitrate. Plant Cell Tiss Org. 2004;77(3):277–81.
Little HA, Papadopoulou E, Hammar SA, Grumet R. The influence of ethylene perception on sex expression in melon ( Cucumis melo L.) as assessed by expression of the mutant ethylene receptor, at-etr1-1, under the control of constitutive and floral targeted promoters. Sex Plant Reprod. 2007;20(3):123–36.
Soldatova NA, Khryanin VN. The effects of heavy metal salts on the phytohormonal status and sex expression in marijuana. Russ J Plant Physiol. 2010;57:96–100.
Martin A, Troadec C, Boualem A, Rajab M, Fernandez R, Morin H, Pitra M, Dogimont C, Bendahmane A. A transposon-induced epigenetic change leads to sex determination in melon. Nature. 2009;461:1135–8.
Boualem A, Troadec C, Camps C, et al. A cucurbit androecy gene reveals how unisexual flowers develop and dioecy emerges. Science. 2015;350(6261):688–91.
Akagi T, Henry IM, Tao R, Comai LA. Y-chromosome–encoded small RNA acts as a sex determinant in persimmons. Science. 2014;346(6209):646.
Pannell JR, Gerchen J. Sex determination: sterility genes out of sequence. Curr Biol. 2018;28(2):R80–3.
Harkess A, Zhou J, Xu C, Bowers JE, Van der Hulst R, Ayyampalayam S, et al. The asparagus genome sheds light on the origin and evolution of a young Y chromosome. Nat Commun. 2017;8(1):1279.
Akagi T, Henry I M, Ohtani H, et al. A Y-encoded suppressor of feminization arose via lineage-specific duplication of a cytokinin response regulator in kiwifruit. Plant Cell. 2018;30(4):tpc.00787.2017.
Diggle PK, Stilio VSD, Gschwend AR, et al. Multiple developmental processes underlie sex differentiation in angiosperms. Trends Genet. 2011;27(9):368–76.
Alvarezbuylla ER, Benítez M, Corverapoiré A, et al. Flower development. Arabidopsis Book. 2010;8(3):e0127.
Roeder AHK, Yanofsky MF. Fruit development in Arabidopsis. Arabidopsis Book 2006;4:e0075.
Lee J, Hassan O, Gao W, et al. Developmental and gene expression analyses of a cotton naked seed mutant. Planta. 2006;223(3):418–32.
Kubo T, Fujita M, Takahashi H, et al. Transcriptome analysis of developing ovules in rice isolated by laser microdissection. Plant Cell Physiol. 2013;54(5):750–65.
Hao S, Ariizumi T, Ezura H. SEXUAL STERILITY is essential for both male and female gametogenesis in tomato. Plant Cell Physiol. 2017;58(1):22–34.
Farbos I, Oliveira M, Negrutiu I, et al. Sex organs determination and differentiation in the dioecious plant Melandrium album (Silene latifolia): a cytological a histological analysis. Sex Plant Reprod. 1997;10(3):155–67.
Lebel-Hardenack S, Hauser E, Law TF, Schmid J, Grant SR. Mapping of sex determination loci on the white campion (Silene latifolia) Y chromosome using amplified fragment length polymorphism. Genetics. 2002;160(2):717–25.
Evans MMS. The indeterminate gamethophyte1 gene of maize encodes a lob domain protein required for embryo sac and leaf development. Plant Cell. 2007;19(1):46–62.
Acosta IF, Laparra H, Romero SP, et al. tasselseed1 is a lipoxygenase affecting jasmonic acid signaling in sex determination of maize. Science. 2009;323(5911):262–5.
Li D, Blakey CA, Dewald C, et al. Evidence for a common sex determination mechanism for pistil abortion in maize and in its wild relative Tripsacum. P Natl Acad Sci USA. 1997;94(8):4217–22.
Pannell J. Mixed genetic and environmental sex determination in an androdioecious population of Mercurialis annua. Heredity. 1997;78(1):50–6.
Chen L, Zhang J, Li H, et al. Transcriptomic analysis reveals candidate genes for female sterility in pomegranate flowers. Front Plant Sci. 2017;8:1430.
Fu WQ, Zhao ZG, Ge XH, Ding L, Li ZY. Anatomy and transcript profiling of gynoecium development in female sterile Brassica napus mediated by one alien chromosome from Orychophragmus violaceus. BMC Genomics. 2014;15(1):61.
Cucinotta M, Colombo L, Roigvillanova I. Ovule development, a new model for lateral organ formation. Front Plant Sci. 2014;5(4):1–12.
Wallander E. Systematics of Fraxinus (Oleaceae) and evolution of dioecy. Plant Syst Evol. 2008;273(1–2):25–49.
Gleiser G, Verdú M. Repeated evolution of dioecy from androdioecy in Acer. New Phytol. 2005;165(2):633–40.
Farbos I, Oliveira M, Negrutiu I, et al. Sex organ determination and differentiation in the dioecious plant Melandrium album (Silene latifolia): a cytological and histological analysis. Sex Plant Reprod. 1997;10(3):155–67.
Yang LL, Chen M, Liu FQ, et al. Study on sepal morphology, metabolize, feature of genetic expression in male flowers of cucumber. Chin Sci Bull. 1999;44:2509–13.
Caporali E, Spada A, Marziani G, Failla O, Scienza A. The arrest of development of abortive reproductive organs in the unisexual flower of Vitis vinifera ssp. silvestris. Sex Plant Reprod. 2003;15:291–300.
Davidson C. An anatomical and morphological study of Datiscaceae. Aliso: A J of Syst Evol Bot. 1973;8(1):49–110.
Listen A, Rieseberg LH, Elias TS. Functional androdioecy in the flowering plant Datisca glomerata. Nature. 1990;343(6259):641–2.
Lü W, Liu WZ. Pollination biology in androdioecious species Tapiscia sinensis (Staphyleaceae). Chin Bull Bot. 2010;45:713–22.
Zhou XJ, Ma L, Liu WZ. Functional androdioecy in the rare endemic tree Tapiscia sinensis. Bot J Linn Soc. 2016;180(4):504–14.
Yang K, Zhou X, Wang Y, et al. Carbohydrate metabolism and gene regulation during anther development in an androdioecious tree, Tapiscia sinensis. Ann Bot. 2017;120(6):967–77.
Manfred GG. Full-length Transcriptome assembly from RNA-Seq data without a reference genome. Nat Biotechnol. 2011;29:644–52.
Pertea G, Huang X, Liang F, et al. TIGR gene indices clustering tools (TGICL): a software system for fast clustering of large EST datasets. Bioinformatics. 2003;19(5):651–2.
Ramoni MF, Sebastiani P, Kohane IS. Cluster analysis of gene expression dynamics. Proc Natl Acad Sci. 2002;99(14):9121–6.
Lu L, Wortley AH, Li DZ, Wang H, Blackmore S. Evolution of angiosperm pollen. 2. The basal angiosperms. Ann Mo Bot Gard. 2015;100:227–69.
Walker JW. Evolution of exine structure in the pollen of “primitive” angiosperms. Am J Bot. 1974;61:891–902.
Muller J. Form and function in angiosperm pollen. Ann Mo Bot Gard. 1979;66:593–632.
Xin GL, Jia GL, Ren XL, Wang YY, Zhao P, Liu WZ. Floral development in the androdioecious tree Tapiscia sinensis: implications for the evolution to androdioecy. J Syst Evol. https://doi.org/10.1111/jse.12517.
Skinner DJ, Hill TA, Gasser CS. Regulation of ovule development. Plant Cell. 2004;16(suppl_1):S32–45.
Eshed Y, Baum SF, Bowman JL. Distinct mechanisms promote polarity establishment in carpels of Arabidopsis. Cell. 1999;99(2):199–209.
Losa A, Colombo M, Brambilla V, Colombo L. Genetic interaction between aintegumenta (ant) and the ovule identity genes seedstick, (stk), shatterproof1, (shp1) and shatterproof2, (shp2). Sex Plant Reprod. 2010;23(2):115.
Galbiati F, Sinha RD, Simonini S, et al. An integrative model of the control of ovule primordia formation. Plant J. 2013;76(3):446–55.
Western TL, Haughn GW. BELL1 and AGAMOUS genes promote ovule identity in Arabidopsis thaliana. Plant J. 1999;18(3):329–36.
Yanofsky MF, Ma H, Bowman JL, Drews GN, Feldmann KA, Meyerowitz EM. The protein encoded by the Arabidopsis homeotic gene agamous resembles transcription factors. Nature. 1990;346:35–9.
Drews GN, Bowman JL, Meyerowitz EM. Negative regulation of the Arabidopsis homeotic gene AGAMOUS by the APETALA2 product. Cell. 1991;65:991–1002.
Ito T, Wellmer F, Yu H, Das P, Ito N, Alves-Ferreira M. The homeotic protein AGAMOUS controls microsporogenesis by regulation of SPOROCYTELESS. Nature. 2004;430:356–60.
L’eon-Kloosterziel KM, Keijzer CJ, Koornneef M. A seed shape mutant of Arabidopsis that is affected in integument development. Plant Cell. 1994;6:385–92.
Brown RH, Nickrent DL, Gasser CS. Expression of ovule and integument-associated genes in reduced ovules of Santalales. Evol Dev. 2010;12:231–40.
Hu YB, Liu W, Xu GH. Research advances in auxin and ethylene signaling and effects of auxin on ethylene response of plants (review). Chinese Bulletin of Botany. 2011;46(3):338–49.
Li WY, Ma MD, Guo HW. Advances in the action of plant hormone ethylene (review). Sci Sinica. 2013;43:854–63.
Lin Z, Alexander LR, Grierson D. LeCTR2, a CTR1-like protein kinase from tomato, plays a role in ethylene signalling, development and defence. Plant J. 2010;54(6):1083–93.
Nemhauser JL, Feldman LJ, Zambryski PC. Auxin and ETTIN in Arabidopsis gynoecium morphogenesis. Development. 2000;127(18):3877–88.
Wu YF, Reed GW, Tian CQ. Arabidopsis microRNA167 controls patterns of ARF6 and ARF8 expression, and regulates both female and male reproduction. Development. 2006;133(21):4211–8.
Bencivenga S, Simonini S, Benková E, Colombo L. The transcription factors bel1 and spl are required for cytokinin and auxin signaling during ovule development in Arabidopsis. Plant Cell. 2012;24(7):2886–97.
Dreni L, Jacchia S, Fornara F, et al. The D-lineage MADS-box gene OsMADS13 controls ovule identity in rice. The Plant J. 2007;52(4):690–9.
Doyle JA. Phylogeny of vascular plants. Annu Rev Ecol Evol S. 1998;29:567–99.
Ross MD. The evolution and decay of overdominance during the evolution of gynodioecy, subdioecy and dioecy. Am Nat. 1980;116:607–20.
Ross MD. Five evolutionary pathways to subdioecy. Am Nat. 1982;119:297–318.
Webb CJ. Empirical studies: evolution and maintenance of dimorphic breeding systems. gender and sexual dimorphism in flowering plants. Springer Berlin Heid. 1999:61–95.
Tanurdzic M, Banks JA. Sex-determining mechanisms in land plants. Plant Cell. 2004;16:S61–71.
Lü W. Pollination biology and maintenance strategy in androdioecious species Tapicia sinensis. Northwest University 2010.
Ma L. Sex allocation when flower and fruit grow synchronously on an androdioecy plant of Tapiscia sinensis (Tapisciaceae). Northwest University. 2013;p.23–24.
Culley TM, Weller SG, Sakai AK. The evolution of wind pollination in angiosperms. Trends Ecol Evol. 2002;17(8):361–9.
Tao ZB, Wortley AH, Lu L, et al. Evolution of angiosperm pollen. 6. The Celastrales, Oxalidales, and Malpighiales (com) clade and Zygophyllales. Ann Mo Bot Gard. 2018;103(3):393–442.
Wallander E. Evolution of wind-pollination and gender specialisation in Oleaceae exaptations and adaptations. Göteborg University, Göteborg, Sweden. 2001.
Ito T, Wellmer F, Yu H, Das P, Ito N, Alves-Ferreira M. The homeotic protein AGAMOUS controls microsporogenesis by regulation of SPOROCYTELESS. Nature. 2004;430:356–60.
Sieber P, Petrascheck M, Barberis A, Schneitz K. Organ polarity in Arabidopsis. NOZZLE physically interacts with members of the YABBY family. Plant Physiol. 2004;135:2172–85.
Liu Z, Yu X, Wang F, Hu S, Liu Y, Lu G. Physiological, biochemical, and molecular characterization of a new female sterile mutant in turnip. Plant Growth Regul. 2012;68(2):239–48.
Lenhard M, Bohnert A, Jürgens G, et al. Termination of stem cell maintenance in Arabidopsis floral meristems by interactions between WUSCHEL and AGAMOUS. Cell. 2001;105(6):805–14.
Balasubramanian S, Schneitz K. NOZZLE regulates proximal-distal pattern formation, cell proliferation and early sporogenesis during ovule development in Arabidopsis thaliana. Development. 2000;127(19):4227–38.
Wei B, Zhang J, Pang C, et al. The molecular mechanism of SPOROCYTELESS/NOZZLE in controlling Arabidopsis ovule development. Cell Res. 2015;25(1):121–34.
Bencivenga S, Simonini S, Benková E, et al. The transcription factors BEL1 and SPL are required for cytokinin and auxin signaling during ovule development in Arabidopsis. Plant Cell. 2012;24(7):2886–97.
Scofield S, Dewitte W, Murray JA. STM sustains stem cell function in the Arabidopsis shoot apical meristem and controls KNOX gene expression independently of the transcriptional repressor AS1. Plant Signal Behav. 2014;9(6):e28934-1-5.
Carles CC, Lertpiriyapong K, Reville K, Fletcher JC. The ULTRAPETALA1 gene functions early in Arabidopsis development to restrict shoot apical meristem activity and acts through WUSCHEL to regulate floral meristem determinacy. Genetics. 2004;167:1893–903.
Scofield S, Dewitte W, Murray JA. The KNOX gene SHOOT MERISTEMLESS is required for the development of reproductive meristematic tissues in Arabidopsis. Plant J. 2007;50(5):767–81.
Azhakanandam S, Nole-Wilson S, Bao F, et al. SEUSS and AINTEGUMENTA mediate patterning and ovule initiation during gynoecium medial domain development. Plant Physiol. 2008;146(3):1165–81.
De Martinis D, Mariani C. Silencing gene expression of the ethylene forming enzyme results in a reversible inhibition of ovule development in transgenic tobacco plants. Plant Cell. 1999;11:1061–72.
Chen H, Sun J, Shuai L, Cui Q, Zhang H, Xin F, et al. An acc oxidase gene essential for cucumber carpel development. Mol Plant. 2016;9(9):1315–27.
Hua J, Meyerowitz EM. Ethylene responses are negatively regulated by a receptor gene family in Arabidopsis thaliana. Cell. 1998;94:261–71.
Shigyo M, Hasebe M, Ito M. Molecular evolution of the AP2 subfamily. Gene. 2006;366(2):256–65.
Bohn-Courseau I. Auxin: a major regulator of organogenesis. CR Biol. 2010;333(4):290–6.
Yamaguchi N, Wu MF, Winter CM, et al. A molecular framework for auxin-mediated initiation of flower primordia. Dev Cell. 2013;24(3):271–82.
Besnard F, Rozier F, Vernoux T. The ahp6 cytokinin signaling inhibitor mediates an auxin-cytokinin crosstalk that regulates the timing of organ initiation at the shoot apical meristem. Plant Signal Behav. 2014;9(6):e28788-1-4.
Goto N, Katoh N, Kranz AR. Morphogenesis of floral ogans in Arabidopsis: predominant carpel formation of the pin-formed mutant. Genes Genet Syst. 2006;66(5):551–67.
Bennett SRM, Alvarez J, Bossinger G, Smyth DR. Morphogenesis in pinoid mutants of Arabidopsis thaliana. Plant J. 2010;8(4):505–20.
He YB, Yan L, Ge CN, et al. PINOID is required for formation of the stigma and style in rice. Plant Physiol. 2019;180(2):926–36.
Aryal R, Ming R. Sex determination in flowering plants: papaya as a model system. Plant Sci. 2014;217–218(1):56–62.
Su YH, Liu YB, Zhang XS. Auxin-cytokinin interaction regulates meristem development. Mol Plant. 2011;04(4):616–25.
Reyesolalde JI, Zúñigamayo VM, Marschmartínez N, Folter SD. Synergistic relationship between auxin and cytokinin in the ovary and the participation of the transcription factor spatula. Plant Signal Behav. 2017;12(10):e1376158.
Das P, Ito N, Alves-Ferreira M, et al. The homeotic protein AGAMOUS controls microsporogenesis by regulation of SPOROCYTELESS. Nature (London). 2004;430(6997):356–60.
Uemura A, Yamaguchi N, Xu Y, et al. Regulation of floral meristem activity through the interaction of AGAMOUS, SUPERMAN, and CLAVATA3 in Arabidopsis. Plant Reprod. 2017;31:89–105.
Sanders PM, Bui AQ, Weterings K, et al. Anther developmental defects in Arabidopsis thaliana, male-sterile mutants. Sex Plant Reprod. 1999;11(6):297–322.
Du XM, Ni XL, Ren XL, et al. De novo transcriptomic analysis to identify differentially expressed genes during the process of aerenchyma formation in Typha angustifolia, leaves. Gene. 2018;662:66–75.
Ye PF, Li M, Liao W, Kai Ge K, Jin SH, Zhang C, Chen XY, Zhaoyu Geng ZY. Hypothalamic transcriptome analysis reveals the neuroendocrine mechanisms in controlling broodiness of Muscovy duck (Cairina moschata). PLoS One. 2019;14(5):e0207050
Zhang Y, et al. Circadian evening complex represses jasmonate-induced leaf senescence in Arabidopsis. Mol Plant. 2018;11(2):326–37.
Mortazavi A, Williams BA, McCue K, et al. Mapping and quantifying mammalian transcriptomes by RNA-Seq. Nat Methods. 2008;5(7):621–8.
Liu Y, Guo CC, Gui-Xia XU, et al. Evolutionary pattern of the regulatory network for flower development: insights gained from a comparison of two Arabidopsis species. J Syst Evol. 2011;49(6):528–38.
Li QL, Liu BS. Genetic regulation of maize flower development and sex determination. Planta. 2017;245:1–14.
Kanehisa M, Araki M, Goto S, et al. KEGG for linking genomes to life and the environment. Nucleic Acids Res. 2007;36(suppl_1):D480–4.
Livak KJ, Schmittgen TD. Analysis of relative gene expression data using real-time quantitative PCR and the 2− ΔΔCT method. Methods. 2001;25(4):402–8.
We acknowledge Dr. Xin Zhang and Yafu Zhou for their valuable discussions.
Funding for this work was supported by the National Natural Science Foundation of China (31770413). Founding body had no role in the design of the study and collection, analysis, and interpretation of data and in writing the manuscript.
Ethics approval and consent to participate
In this study, the project and flower sample collection were permitted by the National Natural Science Foundation of China and the National Nature Reserve Administration of Shennongjia, Hubei, respectively.
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The authors declare that they have no competing interests.
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: Primer sequences and the results of DEGs
GO analysis in M1_vs_H1, M2_vs_H2, and M3_vs_H3.
GO and KEGG pathway enrichment analysis in TERM1 and TERM2.
Figure S1. Differences between mature HF and TYPE III MF. (A) Longitudinal section of HF. (B) Mature embryo sac in HF. (C) In Type III MF, embryo sac development stopped at the triad stage. (D) Longitudinal section of Type III MF. Sy, synergid; sn, secondary nucleus; hy, hypostase; ii, inner integument; oi, uter integument; mi, micropyle. Figure S2. Eight model profoles in TERM1 and TERM2, respectively. In TERM1, the expression patterns of 13,761 genes were analysed, eight model profiles were used to summarize, and five expression patterns of genes showed significant p-values (p < 0.05) (coloured boxes). In TERM 2, the expression patterns of 16,130 genes were analysed, and eight model profiles were used to summarize. Three expression patterns of genes showed significant p-values (p < 0.05) (coloured boxes). Each box represents a model expression profile with the model profile number and p-value. Colored boxes indicate that there are significant differences between floral stages. No color box means no difference. M1, M2 and M3 represent MF at stages 5, 6 and 10, respectively, while H1, H2 and H3 represent bisexual flowers at stages 5, 6 and 10, respectively. The meaning of the ‘significant p-value’ was a significant difference between floral stages. Figure S3. Numbers of differentially expressed genes. (A) TERM1 – trend all by gene number, trend all by P-value. In profile 3: 2364 gene (2.6e-19 P-value) had stable expression in floral stages 5 and 6, but decreased in expression in stage 10; in profile 4, 1664 genes (1.1e-11 P-value) had stable expression in floral stages 5 and 6, but increased in expression in stage 10; in profile 5, 2320 genes (3.7e-17 P-value) increased in expression in floral stages 5 and 6, but decreased in stage 10; in profile 6, 2170 genes (6.2e-06 P-value) had an increased expression in floral stages 5 and 6, but had stable expression in stage 10; in profile 7: 1471 genes (7.7e-18 P-value) had an increased expression in floral stages 5 to 10. (B) TERM2 – trend all by gene number, trend all by P-value. In profile 1, the expression of 2308 genes (3.6e-47 P-value) present the trend of first decline and then maintain stable from stage 5 to 10; profile 6: 3179 genes (1.2e-79 P-value) had an increased expression in floral stages 5 and 6, but had stable expression in stage 10; profile 7: 1839 genes (5.2e-39 P-value), the trend was always upward. (C) GO and KEGG pathway enrichment analysis in TERM1 and TERM2. The meaning of the ‘significant p-value’ was a significant difference between floral stages.
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Xin, G., Liu, J., Liu, J. et al. Anatomy and RNA-Seq reveal important gene pathways regulating sex differentiation in a functionally Androdioecious tree, Tapiscia sinensis. BMC Plant Biol 19, 554 (2019). https://doi.org/10.1186/s12870-019-2081-7
- Morphology and anatomy
- Androdioecious tree
- Tapiscia sinensis
- Sex differentiation
- Transcriptome analysis