Transcriptomic comparison sheds new light on regulatory networks for dimorphic flower development in response to photoperiod in Viola prionantha
BMC Plant Biology volume 22, Article number: 336 (2022)
Chasmogamous (CH)–cleistogamous (CL) dimorphic flowers are developed in Viola prionantha. However, the environmental and genetic factors necessary for the CH–CL transition are unknown.
In the present work, short-day (SD) conditions induced CH flowers, whereas long days (LDs) triggered CL flowers in V. prionantha. Compared to fully developed CH flowers, CL flowers had less mature stamens, no nectar glands, and immature petals. Comparative transcriptomics revealed differentially expressed genes (DEGs) during CL and CH development. Core genes in the photoperiod pathway, such as V. prionantha orthologs of GIGANTEA (GI), CONSTANS (CO), and SUPPRESSOR OF OVEREXPRESSION OF CONSTANS 1 (SOC1), which promote floral induction, were highly expressed in CL flowers, whereas UNUSUAL FLORAL ORGANS (UFO) and B-class MADS-box genes for floral organ identity and development showed an opposite alteration. Moreover, genes in the glycolytic process, sucrose metabolic process, and fatty acid biosynthetic process were all highly expressed in CH flowers. Interestingly, V. prionantha orthologs of the B-class MADS-box genes APETALA3 (AP3) and PISTILLATA (PI) might relate to these sugar–fatty acid processes and were co-expressed with GAIP-B-like and YABBY5 (YAB5), which regulate the development of the petal, stamen, and nectary. Compared to CH flowers, DEGs and hub genes in the most significantly correlated modules of the gene co-expression network, which are involved in abiotic and biotic responses, were upregulated in CL flowers.
We proposed an integrative model for transcription regulation of genes in the photoperiod pathway, floral organ development, stress response, and sugar–fatty acid processes to determine CH–CL flower development in V. prionantha. Particularly, under LDs, activated GI may induce genes involved in the stress-response pathways, and then downregulated AP3 and PI or UFO to inhibit the sugar–fatty acid metabolic processes, together forming CL flowers. In contrast, CH flowers were produced under SDs. This work provides novel insights into the developmental evolution of dimorphic flowers in Viola.
Breeding systems are critical components of a population’s ability to reproduce, and these systems are often involved in the evolution of floral traits to maximize mating opportunities and fertilization success in plants . Cleistogamy is a sexual system in which fertilization within individual closed flowers occurs without pollinator intervention . Cleistogamy, present in 693 angiosperm species, has been classified into three categories, namely dimorphic, complete, and induced cleistogamy, with most (77.3%) being dimorphic . Dimorphic cleistogamy is a specialized form of a mixed-mating system in which a single plant produces both open, potentially outcrossed chasmogamous (CH) and closed, obligately self-pollinated cleistogamous (CL) flowers. Moreover, the CL flower is a structurally modified form of the CH flower for autogamy [4, 5]; it never opens, and self-pollination occurs in a bud-like stage that is reduced compared with CH flowers. The nectar and odors of CL flowers are absent, petals are rudimentary or completely missing, stamens are often reduced in both number and size, and there are few pollen grains [6,7,8,9].
Several hypotheses have been proposed to explain natural selection leading to the maintenance of mixed-mating strategies of CH–CL flowers. In the reproductive assurance hypothesis, CL flowers are considered a backup mechanism of reproduction if CH flowers fail to set seeds, thereby extending the reproductive window of CH/CL species during the growing season [3, 10,11,12,13]. Hypothetically, to prevent inbreeding depression in dimorphic cleistogamy, CH flowers are advantageous in that they promote outcrossing and gene-flow within and among populations and produce genetically diverse progenies, thus maintaining genetic diversity, while CL increases a populations’ susceptibility to genetic drift and inbreeding depression if deleterious alleles cannot be purged [3, 11, 14,15,16]. The resource allocation hypothesis suggests that allocating resources to different floral morphs optimizes the use of available energy reserves [17, 18], and the production of two floral morphs is independent of each other, but one or both are correlated with a resource, typically size [19, 20] or pollinator availability . CH flowers have a high energetic cost of production in some species and rely on pollinators for fertilization [3, 21]. A complex habitat model suggests that heterogeneity in the environment may lead to phenotype selection and that the frequencies of CH and CL flowers depend on environmental conditions . Various environmental factors, such as photoperiod [2, 9], light intensity , nutrient availability , water supply , and temperature , influence the type of flowers produced.
The genus Viola (true violets) is well known for its large number of species displaying a CH/CL mixed breeding system [2, 3, 9, 16]. CH and CL flowers can exhibit different light intensities, as seen in Viola pubescens. As the average light quantity decreases, the odds of a CH bud developing decrease, while the odds of a CL bud increase . Viola philippica CH flowers are induced under short-day (SD) conditions, and photoperiod extension is intended to induce CL flower formation [9, 23]. Viola prionantha is a perennial herb that can also develop both CH and CL flowers. However, how environmental and genetic factors affect dimorphic flower development remains unknown in this species. In this study, we observed floral development under different photoperiods in V. prionantha and compared transcriptomic variations based on full-length transcriptomes. The aims of this study were (1) to reveal the role of the photoperiod in dimorphic flower development, (2) to identify differentially expressed genes (DEGs) during CH and CL flower development, and (3) to investigate gene regulatory pathways that might determine the patterning and processes of CH and CL development. Our study contributes to the understanding of the molecular basis underlying the developmental evolution of environmentally dependent mating systems in Viola.
Morphology of CH and CL flowers in V. prionantha.
V. prionantha is a perennial plant that can develop both CH and CL flowers at different times during the flowering season. This is quite similar to observations in V. philippica . CH flowers of V. prionantha had also five large and purple petals, with the lowest petal protruding slightly at the base into a spur, and five stamens forming a cone surrounding the pistil (Fig. 1A and B). Each stamen of V. prionantha had four pollen sacs, and the lowest two stamens were attached to noticeable nectar glands (Fig. 1C). The style of the pistil was erect and exceeded the stamens (Fig. 1D). In contrast, CL flowers of V. prionantha had two stamens without nectar glands, each stamen had two pollen sacs, and the five petals were all undeveloped as primordial structures (Fig. 1E–G). The style of the pistil was curved and bent to the two big stamens (Fig. 1H). Under certain conditions, intermediate CL (inCL) flowers developed in V. prionantha, and they displayed variable characteristics. Typical ones included one to three poorly developed petals, two to five developed stamens, and a curving style of the pistil (Fig. 1I–K). Therefore, the number and size of petals and stamens in CL and inCL flowers were smaller than those of normally developed CH flowers in V. prionantha. In addition, the filaments of CL and inCL stamens were distinct compared to that of CH flowers in V. prionantha, in which they were undetectable (Fig. 1C,G and J).
Photoperiod affects CH–CL flower development
Under natural conditions, V. prionantha developed complete CH flowers in the early spring and a mixture of inCL and CH flowers in the late spring, whereas complete CL flowers was produced in the summer and early autumn, suggesting that dimorphic flower development in this species might be regulated by the photoperiod. We thus used three photoperiods (10-, 12-, and 16-h daylight) to test this assumption in V. prionantha. The results demonstrated that complete CL flowers were formed under 16-h daylight, and both inCL and CH flowers were simultaneously developed at 10–12-h daylight in V. prionantha. Under a photoperiod of 10-h daylight, > 80% of the floral buds were developed to be CH flowers (Fig. 1L). The CH-CL formation pattern of V. prionantha in response to photoperiods is also similar to that in V. philippica . In addition, flowering was induced as the photoperiod was extended in V. prionantha (Fig. 1M).
Upon naked-eye visualization of the floral buds, roughly five floral developmental stages (S1–S5) were defined in V. prionantha for both CH flowers under 10-h daylight (Fig. 1N–R) and CL flowers under 16-h daylight conditions (Fig. 1S–W). At S1, CH flowers had five obvious petals and stamens (Fig. 1N), whereas CL flowers had two stamens, and other stamens and all petals were retained as organ primordial structures (Fig. 1S). At S2, four whorl floral organs of CH flowers continued to develop, and the style of the pistil was higher than that of the stamens. The nectar glands at the base of the two stamens and spur of lower petals began to appear, while the style of the pistil in CL flowers began to bend to the two developed stamens (Fig. 1O and T). At S3, the nectar glands at the base of the two stamens were more obvious in the CH flowers, while the five petals and the other three stamens remained in the organ primordial state, and the filaments of stamen were more distinct in the CL flowers (Fig. 1P and U). At S4, the petals turned pink in the CH flowers, the filaments of the stamens became longer and finer, and the stamens were closer to the pistil in the CL flowers (Fig. 1Q and V). At S5, the petals turned purple, and the stamen cap became yellow in the CH flowers, while in the CL flowers, the stamen cap also became yellow, and the development of the three stamens and all petals was completely arrested as primordial structures (Fig. 1R and W).
To further reveal the effect of the photoperiod on CH and CL flower development, the photoperiod of V. prionantha plants was interconverted between 16- and 10-h daylight. In both cases of the “10-h to 16-h” daylight shift (Figure S1A–E) and “16-h to 10-h” daylight shift (Figure S1F–J), the CL or CH flower buds that had been induced in their original photoperiod continued to develop as their pre-programmed developmental trajectory in the new environment. Statistical analyses demonstrated that, within 8 days after the environment shift, the newly induced flower buds showed a series of inCL flower types, whereas buds initiated 8 days after the environment shift were directly transformed into CL flowers or CH flowers corresponding to the ultimate conditions of 16- or 10-h daylight (Figure S1K–P). These results indicate that the photoperiod regulates CH–CL flower development and transition in V. prionantha, and the long-day (LD) conditions can inhibit the development of stamens and petals. To understand the molecular basis for the dimorphic flower development or the CH–CL transition, we performed comparative transcriptomics between CL and CH flowers in V. prionantha.
Transcriptome sequencing and functional annotation
We first sequenced the full-length transcriptome of V. prionantha of whole plants, including the roots, stems, leaves, and involved floral buds, using the Pacific Biosciences Sequel platform, and generated 1,021,145 reads in total (Fig. 2A, Table S1). There were 155,918 full-length non-chimeric and clean reads, and 42,765 consensus isoforms were identified (Fig. 2A). The mean and N50 of the isoform length were 2346 bp and 3669 bp, respectively (Fig. 2A, Figure S2A). Functional annotations of the longest open reading frame (ORF), as the coding sequence (CDS), were performed using BLAST, Blast2GO, and InterProScan5, and 98.15% of transcripts were annotated (Fig. 2A, Tables S2 and S3). The NR database had the highest annotation rate, accounting for 96.1% of all transcripts, and the GO database had the lowest annotation rate, accounting for 35.39% of all transcripts (Table S3). The total number of transcripts annotated by all seven databases was 17,102, accounting for 40.74% of all transcripts (Figure S2B). With NR annotation, approximately 74% of all transcripts of V. prionantha were similar to Jatropha curcas, Populus trichocarpa, P. euphratica, and Ricinus communis (Figure S2C). To reveal the evolutionary relationship of V. prionantha, we first used Orthofinder to identify orthologous genes in the amino acid sequences of 17 other plant species, including P. deltoids, P. trichocarpa, and Arabidopsis thaliana, and a total of 24,585 gene orthogroups were constructed (Table S4). Phylogenetic analysis with these orthologous sequences using H. vulgare and O. sativa as an outgroup supported the notion that V. prionantha was the closest relative to P. deltoides and P. trichocarpa (Figure S3). We then evaluated the expansion and contraction of certain gene families and found that a total of 2555 families were expanded (73 significant, P ≤ 0.05), while 4586 gene families were contracted (120 significant, P ≤ 0.05) in V. prionantha (Figure S3). GO and KEGG enrichment analyses of the 1405 genes in the significantly expanded gene families (Table S5) revealed GO (Figure S4A, Table S6) and KEGG (Figure S4B, Table S6) categories/pathways, including ethylene-responsive proteins, lipoxygenase, and jasmonate ZIM domain protein, that might be involved in stress response and flower development.
RNA-seq between CH and CL flowers
To observe general variation patterns at the transcriptomic level between CH and CL flowers, three developmental stages (CH1-3 or CL1-3) of each flower type, corresponding to S1, S3, and S5, were subjected to RNA-seq analysis. We sequenced the 18 samples using the BGISEQ-500 platform and generated approximately 23.98 Mb RNA clean reads per sample on average (Table S7). By mapping them to the identified unique isoforms, 67.62% of the RNA clean reads were reasonably aligned (Table S8). Moreover, most transcripts were completely covered with uniform read coverage alone in the body using the RNA-seq data (Figure S5A and B). Gene expression correlation with samples showed that the samples in the three biological repeats at the same developmental stage had a high correlation, whereas the samples in different developmental stages had a relatively low correlation (Fig. 2B). Principal component analysis (PCA) also showed that three repeated samples at the same developmental stage were clustered together, whereas the samples at different stages were far away from each other (Fig. 2C). Thus, all generated RNA-seq data could be used for further analysis.
GO enrichment of stage-specific DEGs between CH and CL flowers
To identify genes related to dimorphic floral development in V. prionantha, we performed a DEG analysis by comparing the CH and CL flowers for the developmental stages (S1, S3, and S5) with DESeq2. A total of 162, 673, and 1716 genes were respectively found to be differentially expressed in S1, S3, and S5 (Table S9), and a Venn diagram revealed the distribution and relationship of these DEGs among these three developmental stages (Figure S6A). To further reveal the contribution of the DEGs’ variation to the CH-CL floral transition, we investigated the potential biological functions of the stage-specific DEGs through GO enrichment analysis.
In S1, eight enriched GO terms were constructed with 162 DEGs between the CH and CL flowers, and the most dominant was transcription regulation (Fig. 3A, Figure S6A, Table S10). Of these, 5 genes were downregulated and 14 genes were upregulated in CL flowers relative to CH flowers. The genes downregulated in CL flowers included four B-class MADS-box genes PISTILLATA (PI, Vp42765), APETALA3 (AP3, Vp31710, Vp32333, Vp33366), and one F-box transcription factor (TF) gene UNUSUAL FLORAL ORGANS (UFO, Vp21783) (Figure S6B), which might be critical for promoting the initiation and development of petals and stamens (Table S11). While the 14 upregulated TF genes in CL flowers included SUPPRESSOR OF OVEREXPRESSION OF CONSTANS 1 (SOC1, Vp24825), FLAVIN-BINDING KELCH REPEATF-BOX1/ ADAGIO3 (FKF1/ADO3) (Vp13028), ETHYLENE RESPONSE FACTOR53 (ERF053) (Vp15804, Vp19048), and ERF4 (Vp23464) (Figure S6B), which might be related to the circadian clock, carbohydrate synthesis, and defense response (Table S11).
A total of 23 enriched GO terms were identified for the 571 DEGs specific in S3 relative to S1, which mainly included defense response, carbohydrate metabolic process, nitrate assimilation, sporopollenin biosynthetic process, calcium ion transport, fatty-acyl-CoA biosynthetic process, glucose catabolic process, and jasmonic acid-mediated signaling pathways (Fig. 3B, Figure S6A, Table S10). Notably, 17 DEGs were involved in the defense response, and they were all upregulated in CL flowers compared with CH flowers (Fig. 3B). Of these, 16 DEGs involved in the carbohydrate metabolic process included 7 downregulated genes and 9 upregulated genes in CL flowers (Fig. 3B). In addition, genes in sporopollenin biosynthetic, fatty-acyl-CoA biosynthetic, and glucose catabolic processes were downregulated in CL flowers compared with CH flowers, and genes in nitrate assimilation and calcium ion transport were upregulated in CL flowers (Fig. 3B).
A total of 33 enriched GO terms were identified for the 1331 specific DEGs in S5 and included genes in the glycolytic process, carbohydrate metabolic process, and fatty acid biosynthetic process (Fig. 3C, Figure S6A, Table S10). Most of these genes were downregulated in CL flowers compared with CH flowers, whereas the genes involved in temperature compensation of the circadian clock were upregulated in CL flowers compared with CH flowers (Fig. 3C).
Taken together, the number of DEGs increased as the flower developed. The differentially expressed TF genes occurred at the earlier stages, and then the genes involved in metabolic processes related to sugar and fatty acids became differentially expressed between CH and CL flowers at late developmental stages, implying the essential role of these DEGs and their programmed regulation in the divergence of CH and CL flowers in V. prionantha.
Expression patterns of MADS-box genes in V. prionantha.
Downregulation of B-class MADS-box genes induces CL flowers in V. philippica . The downregulated genes enriched in the regulation of transcription were mainly B-class MADS-box genes. We therefore characterized this gene family and obtained 23 MIKC-type MADS-box genes from the whole transcript data of V. prionantha. Phylogenetic analysis showed that the MADS-box genes of V. prionantha always clustered with their homologous genes in A. thaliana (Figure S7), suggesting their orthology. An expression profile of the identified MADS-box genes in three developmental stages of CH and CL flowers in V. prionantha showed that a high level of expression of the four B-class MADS-box genes VprAP3 (Vp31710, Vp32333, Vp33366) and VprPI (Vp42765) was observed in CH flowers relative to CL flowers (Fig. 4A, Table S12). In addition, the level of expression of the C-class MADS-box gene AGAMOUS (AG, Vp28027) was also higher in the CH flowers. However, the photoperiod-induced genes, such as SOC1 (Vp24825) and FRUITFULL (FUL, Vp29424), D-class MADS-box gene SEEDSTICK (STK, Vp30579), and AGAMOUS-LIKE6 (AGL6, Vp28883, Vp37510), showed lower expression levels in CH flowers than in CL flowers (Fig. 4A, Table S12).
We focused particularly on genes co-expressed with VprAP3/VprPI. A total of 37 genes showed the highest correlation (PCC > 0.9) with VprAP3/VprPI expression (Fig. 4B, Table S13). GO enrichment analysis showed that these genes were mainly involved in the fatty acid biosynthetic process, glycolytic process, carbohydrate metabolic process, glucose metabolic and catabolic process, positive regulation of flower development, and pollen development (Fig. 4C, Tables S14 and S15). Moreover, the expression of most genes co-expressed with VprAP3 and VprPI was higher in CH flowers of the three developmental stages than in CL flowers (Figure S8). The results suggested that glycolytic, fatty acid biosynthetic, and carbohydrate metabolic processes were putatively controlled by VprAP3/VprPI for dimorphic flower development. In addition, VprAP3/VprPI were also co-expressed with GAIP-B-like (Vp14987) and YABBY5 (YAB5, Vp31665) genes that regulate the development of petals, stamens, and nectaries (Fig. 4C, Table S15).
Expression profile of genes related to sugar–fatty acid processes in V. prionantha.
Genes involved in sucrose metabolic, glycolytic, and fatty acid biosynthetic processes were highly expressed in CH flowers compared to CL flowers, especially at S5 (Fig. 3C, Table S10). A higher expression level of sucrose metabolic process genes, i.e., SUCROSE-PHOSPHATE SYNTHASE 1 (SPS1, Vp9177, Vp9309) and SPS3 (Vp10032), which encode the key enzymes for sucrose synthesis, was observed in CH flowers than in CL flowers (Fig. 5A, Table S16). In the GO term of the glycolytic process, 16 genes were significantly differentially expressed, and most of them were upregulated in CH flowers at three developmental stages compared to CL flowers (Fig. 5B, Table S16).
Twenty-eight genes in the fatty acid biosynthetic process were significantly differentially expressed between the CH and CL flowers (Fig. 5C). The expression level of genes encoding biotin carboxyl carrier protein 2 (BCCP2, Vp25917), ketoacyl-CoA synthase (KCS, Vp15066, Vp19527, Vp30421, Vp19022, and Vp13523), and long-chain acyl-CoA synthetase (LACS, Vp13395, Vp14397, Vp15333, and Vp17649) participating in fatty acid biosynthesis was stably higher in CH flowers than in CL flowers during development, while LINOLEATE 9S-LIPOXYGENASE 5 (LOX1.5, Vp10416) was less expressed in CH flowers than in CL flowers (Fig. 5C, Table S16). Moreover, the expression of genes involved in lignin and cutin synthesis, such as COUMARATE—COA LIGASE (4CLL1, Vp19273, and Vp19820), was also constitutively higher in CH flowers than in CL flowers during development (Fig. 5C, Table S16). These results suggest that CH floral development might require more fatty acids, which could promote stamen fertility, increase the osmotic pressure of stamens and petals, and absorb and transport metal ions in floral organs (Table S16).
Additionally, there were 45 DEGs in the carbohydrate metabolic process, of which 14 genes were downregulated and 31 genes were upregulated in CH flowers compared to CL flowers (Fig. 5D). Most gene-related glycosidase families, including xylosidase (Xyl, Vp13859, Vp14913, Vp15375, Vp15991, and Vp16204), Glucan endo-1,3-beta-glucosidase (GLC1, Vp25276), and cellulose1 (CEL1, Vp40938), were stably downregulated in CH flowers compared to CL flowers, whereas polygalacturonase (PG) genes, including Vp34857, Vp39992, Vp24046, and Vp14690, were upregulated in CH flowers (Fig. 5D, Table S16).
Gene co-expression networks during CH–CL flower development
To facilitate the understanding of the regulatory network of flowering interconversion, we built weighted gene co-expression networks with all DEGs (2064 genes) among the three different developmental stages of V. prionantha. We chose a power of β = 10 based on the scale-free topology criterion to generate a hierarchical clustering tree (Figure S9A and B). A total of five co-expression modules (mergeCutHeight = 0.2) M1–M5 marked with different colors were ultimately identified, and they had a gene number in a module ranging from 71 to 969 (Fig. 6A). Correlations between the modules’ eigengenes (MEs) and genotypes/stages showed that all modules were obviously correlated with flower phenotypes, and M1 (383 genes) and M2 (478 genes) modules exhibited the most significant correlation (Fig. 6B). Significant correlations were also detected between stage-specific gene expression and module membership (MM) in each module (Figure S10), particularly in M1 and M2 modules (Figure S10A and B). Therefore, genes in M1 and M2 might play a role in CH–CL flower development. GO annotations revealed that most genes in M1 were involved in defense response, cellulose biosynthetic process, response to oxygen-containing compounds, response to karrikin, regulation of transcription, lipid metabolic process, and carbohydrate metabolic process (Fig. 6C, Table S17). The top 10 enriched GO terms in M2 were related to the response to jasmonic acid, response to fungus, response to blue light, regulation of transcription, protein dephosphorylation, positive regulation of LD photoperiodism, and flowering (Fig. 6D, Table S18).
To further identify the key genes essential for CH–CL flower development, we extracted hub genes in the M1 and M2 modules. The top 20 genes with the highest maximum clique centrality (MCC) values were considered hub genes (Fig. 6E and F, Tables S19 and S20). For instance, genes in M1, including HOMEOBOX-LEUCINE ZIPPER PROTEIN 12 (ATHB-12), PHYTOCHROME A SIGNAL TRANSDUCTION 1 (PAT1), MYB44, SENESCENCE-ASSOCIATED GENE 101 (SAG101), and GERMIN-LIKE PROTEIN 6 (GLP6), were responsible for abiotic and biotic stress in other plant species (Fig. 6E, Table S21), while genes in M2, including ERF4 and XYLOGLUCAN ENDOTRANSGLUCOSYLASE/HYDROLASE 23 (XTH23), were also related to stress responses (Fig. 6F, Table S21). Notably, a hub gene Vp8612 encoding V. prionantha GIGANTEA (VprGI) was found in M2, and this gene belonged to the GO terms of positive regulation of LD photoperiodism flowering (Fig. 6F, Table S21). These genes were expressed at a low level in CH flowers compared with CL flowers (Figure S11A and B). We then focused particularly on the VprGI co-expression network in V. prionantha. The expression of 17 genes showed the highest correlation (PCC > 0.8, MR ≤ 10) with VprGI expression (Fig. 6G, Table S22), and they included V. prionantha CONSTANS (VprCO), PSEUDO-TYPE RESPONSE REGULATORS1 (APRR1), LATE ELONGATED HYPOCOTYL (LHY), EXOCYST COMPLEX COMPONENT 70B1 (EXO70B1), ERF4, PBS1-like kinases 8 (PBL8), and PXY-correlated (PXC3), which are involved in the circadian clock and defense response progress (Table S23). The expression of these genes, except for LHY, was at low levels in CH flowers relative to CL flowers (Fig. 6H). In addition, PHOSPHOMETHYLPYRIMIDINE SYNTHASE (THIC), which plays an important role in linking the circadian clock and metabolic rhythm, was also at low levels in CH flowers relative to CL flowers in V. prionantha (Table S23).
The results suggest that LD light could induce the co-expression of floral inducers, such as VprGI and VprCO, and coincidently stress-response genes during the induction of CL flowers in V. prionantha.
Expression of key TF genes correlated with CH–CL development
Six key candidate regulatory genes (GI:Vp8612, CO:Vp14425, SOC1:Vp24825, UFO:Vp21783, AP3:Vp33366, and PI:Vp42765) in V. prionantha that might be essential for CH–CL floral transition were targeted and designated VprGI, VprCO, VprSOC1, VprUFO, VprAP3, and VprPI, respectively. Their expression variations during CH and CL development were validated using qRT-PCR. The expression of VprGI, VprCO, and VprSOC1 was at high levels in CL flowers under 16-h daylight relative to those subjected to 12- and 10-h daylight, whereas the expression of VprUFO, VprAP3, and VprPI was at high levels in CH flowers under 10-h daylight relative to inCL and CL flowers under 12- and 16-h daylight (Fig. 7A–C, Table S24). These results were consistent overall with the transcriptome data. We also investigated the expression of these genes in V. prionantha plants under 10-h daylight after they were switched to 16-h daylight conditions. The expression of VprGI, VprCO, and VprSOC1 in the first and second stages of floral buds were elevated with continuous increasing illumination and became significantly upregulated after a one-day shift from 10- to 16-h daylight, while expression variation of VprUFO, VprAP3, and VprPI showed the opposite trend (Fig. 7D, Table S24).
CH flowers possess colored petals and nectar to attract pollinators, while CL flowers are obligate self-pollinators with vestigial or undeveloped petals, and no nectar. The petal and stamen primordia were initiated, and further development was arrested during CL floral development. No morphological differences at floral induction or floral organogenesis were observed between CH and CL flowers in V. prionantha, and flower morphological differentiation in V. prionantha of the two flower types should be determined after floral organogenesis. This is similar to observations in V. philippica . In response to the photoperiod, GAs interact with B-class homeotic genes and regulate dimorphic flower development in V. philippica . In the present work, the photoperiod played a role in CH–CL development. Although no differential expression of GA-biosynthetic genes was found (this might be due to the sampling strategy), we revealed several novel findings at transcriptomic levels. We proposed an integrative role for transcription regulation of genes involved in photoperiod–circadian pathways, organ development, stress response, and sugar–fatty acid metabolic processes in response to photoperiod for CH–CL development, shedding new light on the understanding of the molecular basis underlying the developmental evolution of CH–CL transition in V. prionantha.
Photoperiod regulates dimorphic flower development in V. prionantha
Many environmental factors can affect CH–CL development [8, 9, 22]. The CH/CL system is favored in a heterogeneous parental environment if individuals are exposed to a selection regime in which each flower type is favored in a particular environment . The photoperiod can influence the timing of the floral transition, which leads to the conversion of the shoot apical meristem into a floral meristem and subsequently to the formation of flowers in plants [24, 25]. Our study showed that photoperiod also affected dimorphic flower development, and the phenology of the two flower types in V. prionantha was mainly determined by photoperiod. SD light induced CH flower development, whereas LD light induced CL flower development. This phenomenon was also observed in other Viola species, such as V. odorata and V. philippica [2, 9]. Moreover, when the V. prionantha plants with CL flowers under LD light or CH flowers under SD light were interconverted, the newly induced flowers showed a series of inCL flower types, and finally transformed into CH flowers or CL flowers. The transition depended on the duration of the photoperiod in the new environment in a manner of “the longer, the more thorough.” Therefore, the photoperiod regulates dimorphic flower formation in V. prionantha.
Transcription regulation of CH and CL development in V. prionantha
Gene expression variation in response to photoperiod variation is the major molecular basis underlying the formation of CH or CL flowers. Driven by this presumption, we comparatively investigated the transcriptomic variations. In line with the morphological variation pattern, relatively fewer genes were identified as DEGs in the earlier developmental stages, while more genes became DEGs as the developmental course advanced. Moreover, transcription regulation was different in the early stages, while the genes involved in metabolic processes diverged in the later developmental stages. Similarly, the DEGs in stage 1 were mainly involved in the regulation of transcription. B-class MADS-box genes VprAP3 and VprPI and one F-box TF gene VprUFO were obviously upregulated in CH flowers compared with CL flowers in V. prionantha.
The floral ABC model explains how three major function class genes (A-, B-, and C-class) specify the identity of the four floral organ types. A function specifies sepal identity [26, 27], while A and B activities together specify petal identity [26,27,28,29]. B plus C activity specifies stamens , while C activity specifies carpel identity . A pair of MADS-box genes, AP3 and PI, in Arabidopsis encode B-function activity [32, 33]. B-class MADS-box genes are involved not only in the specification of organ identity of petals and stamens but also in the control of organ maturation [9, 34, 35]. In V. philippica, the downregulation of B-class MADS-box genes during the late developmental stages may result in organ size reduction and developmental abortion, and the expression of these genes is induced by SDs and inhibited by LDs . A similar expression variation of B-class genes during CH–CL development was observed in V. prionantha. Therefore, LDs could also inhibit the development of petals and stamens by directly or indirectly inhibiting the expression of VprAP3 and VprPI genes, thus producing CL flowers in V. prionantha. In particular, GAIP-B-like and YAB5 were co-expressed with VprAP3 and VprPI, and they were upregulated in CH flowers compared with CL flowers in V. prionantha. GAIP-B-like encodes the DELLA protein, regulates the expression of AP3, and is involved in petal and stamen development . YAB5 is indispensable for pseudonectary development . These results further support the transcription regulation of B-class MADS-box genes in CH–CL development.
UFO is not a component of the floral ABC model. However, it is required to initiate the floral program . UFO is expressed in the early development of petals and stamens in Arabidopsis, probably restricting the B-class MADS-box genes’ expression domain to these organs [39, 40]. Moreover, UFO expression is also required for normal petal blade outgrowth after petal identity has been established . Furthermore, UFO is involved in activating CRABS CLAW (CRC) during nectary and carpel development . We showed that VprUFO was significantly upregulated in CH flowers compared with CL flowers, especially at stage 1, and induced by SD light. Therefore, the photoperiod may, directly or indirectly, regulate VprUFO, which is further involved in influencing VprAP3 and VprPI, thus controlling petal and stamen development of either CH or CL flowers in V. prionantha.
Role of genes in sugar–fatty acid metabolic processes in dimorphic flower development
Sugar and fatty acids play important roles in floral development and function, for example, flower opening [43, 44]. The expression of most genes in the glycolytic, fatty acid biosynthetic, and sucrose metabolic processes was higher in CH flowers than in CL flowers, especially at the third developmental stage. Moreover, genes co-expressed with VprAP3 and VprPI involved in the glycolytic, fatty acid biosynthetic, and sucrose metabolic processes were stably higher in CH flowers than in CL flowers throughout development. Therefore, B-class MADS-box genes might be involved in regulating sugar–fatty acid processes, thus playing a role in determining CH or CL under different photoperiods. However, evidence of the regulation of sugar–fatty acid metabolism by B-class MADS-box genes has not yet been reported, which requires investigation.
It is worth mentioning that PG and Xyl not only participate in the carbohydrate metabolic process but are also involved in flower development. Overexpressing PG displays higher proportions of flowers with extra petals, suggesting PG involvement in floral organ patterning , while the knockout of Arabidopsis PG genes results in the generation of tetrad pollen . The expression of PG (Vp34857, Vp39992, Vp24046, and Vp14690) was low in CL flowers and higher in CH flowers. Xyl acts on xyloglucans in the cell wall to promote cell expansion, which might involve the elongation of anther filaments and the degradation of anthocyanin [47, 48]. In the present study, a high level of expression of Xyl2 (Vp13859, Vp14913, Vp15375, Vp1599, and Vp16204) was observed in CL flowers, with a low level in CH flowers. The results suggested that Xyl2 might be involved in the elongation of anther filaments and the degradation of anthocyanin in CL flowers of V. prionantha.
Our results showed a correlated variation between sugar–fatty acid metabolic gene expression and flower types, implying the role of sugar–fatty acid metabolism in dimorphic flower development.
Gene co-expression of the photoperiod pathway and defensive responses
Many genes in the photoperiod pathway related to the circadian clock are involved in flower induction, such as GI, FKF1/ADO3, CO, FT (FLOWERING LOCUS T), FUL, and SOC1 in Arabidopsis. The expression profile of GI is controlled by the circadian clock, and the GI protein is required for the function of FKF1 in regulating CO transcription [49,50,51]. CO plays a central role in activating FT expression for the induction of SOC1. SOC1 promotes floral transition [52, 53], which is, in part, activated by the floral identity gene LEAFY (LFY) [54,55,56]. Furthermore, FUL has been shown to promote flowering in a partially redundant manner with SOC1 . In V. prionantha, the expression of genes controlled by the circadian clock was at a high level in CL flowers relative to CH flowers. The study showed that LDs induced the V. prionantha to bloom earlier, probably because LD promoted the expression of the orthologous genes of GI, FKF1/ADO3, CO, FUL, and SOC1 in V. prionantha.
The present study showed that 17 DEGs in S3 involved in the defense response were upregulated in CL flowers compared with CH flowers. Moreover, the LOX (lipoxygenase) gene family in V. prionantha was significantly expanded, and the level of expression of LOX1.5 was lower in CH flowers than in CL flowers. LOX, which are precursor molecules of JA biosynthesis, are involved in stress responses and filament development in flowers [58, 59]. Furthermore, most of the hub genes in module1 and module2 of WGCNA responded to abiotic and biotic stress, such as ATHB-12, MYB44, PAT1, SAG101, GLP6, ERF4, and XTH23, and the level of expression of these genes was higher in CL flowers than in CH flowers at three development stages.
Interestingly, except for circadian clock genes, genes in the VprGI co-expression network were resistant to stress, such as EXO70B1, ERF4, PBL8, and PXC3, and these genes were expressed at a high level in CL flowers compared with CH flowers. Moreover, the gene family of the response to ethylene in V. prionantha was also significantly expanded, and ERF4 belongs to the ethylene response factor . Co-expression of VprGI and defense response genes indicates that these stress-response genes might be controlled by VprGI or other circadian clock genes in V. prionantha. The circadian clock genes respond to various abiotic and biotic stressors in A. thaliana and crops , and Arabidopsis GI is involved in signaling pathways for various abiotic stressors [62, 63]. For example, the EEL (ENHANCED EM LEVEL)-GI complex positively regulates diurnal ABA synthesis by affecting the expression of NCED3 (9-CIS-EPOXYCAROTENOID DIOXYGENASE 3) and contributes to drought tolerance in Arabidopsis . In addition, the GI-mediated regulation of CDFs (CYCLING DOF FACTOR) contributes to the response to freezing temperatures . Therefore, circadian clock stress-response gene modules might be involved in CH–CL development in V. prionantha.
A novel integrative model for CH–CL development
In Arabidopsis, LD light induces flowering induction genes, such as GI, FKF1/ADO3, FT, CO, SOC1, and AGL24, and these proteins in turn promote the expression of flower meristem genes LFY and AP1 . Once the floral meristem has been specified, AP1 and LFY activate floral organ identity genes , LFY participates with UFO in the regulation of AP1 and AP3 transcription [39, 40], and WUS co-regulates the expression of AG [65, 66]. However, in V. prionantha, LDs also induced the expression of VprGI, VprFKF1/ADO3, VprCO, and VprSOC1, but the expression of VprAP1, VprAP3, and VprAG was not promoted but repressed, thus producing CL flowers. The opposite variation was observed under SD, thus producing CH flowers. Coincidently, the co-expression of circadian clock-related genes and stress-response genes in the photoperiod pathway indicated that circadian clock genes could promote stress-response genes under LDs, which could inhibit the expression of genes related to floral organ development, especially VprUFO, VprAP3, and VprPI. Similarly, cis-elements of stress responses, such as abscisic acid, drought, low-temperature response, and anaerobic response, were prevalent in the promoters of VprAP3 and VprPI in V. prionantha (Table S25). Moreover, circadian-regulated GI is involved in signaling pathways for various abiotic stressors [62, 63]. In this scenario, energy was consumed to respond to the activation of abiotic and biotic stress genes; it would require less energy to trigger the expression of genes related to CH flower development, which is an energy-consuming process. Therefore, in response to LD, stress-response genes could be induced by VprGI, which might downregulate the expression of VprAP3 and VprPI (Fig. 8). We also found that genes significantly co-expressed with VprAP3 and VprPI were involved in glycolytic and fatty acid biosynthetic processes, and they were highly expressed in the floral buds induced under SDs, which might contribute to CH flower development (Fig. 8). Furthermore, the final and intermediate products of the glycolytic process and fatty acid biosynthetic process include the terpenoid, fatty acid, and phenolic compounds that are necessary for later flower development . In addition, some genes related to cellulase involved in sugar–fatty acid processes, such as GLC1 and CEL1, were expressed at high levels in CL flowers compared to CH flowers. The biochemical products of GLC1 and CEL1 encoding enzymes act as osmoprotectants, playing important roles in abiotic or biotic stress resistance [68,69,70,71]. Therefore, the photoperiod might regulate genes in the photoperiod pathway controlling flowering time, circadian clock-related genes, and floral organ identity genes without affecting floral organ initiation, and the involved transcription factors could further regulate genes involved in stress response and sugar–fatty acid metabolic processes, suggesting that their products serve as downstream molecules to determine whether there are CH flowers under SDs or CL flowers under LDs.
The photoperiod drives or regulates the development and transition of CH–CL flowers in V. prionantha. SDs induced CH flower development, whereas LDs induced CL flowers. LDs induced earlier bloom and promoted the expression of the orthologous genes of GI, FKF1/ADO3, APRR1, CO, FUL, and SOC1 in V. prionantha, whereas SDs promoted the expression of VprUFO and B-class MADS-box genes. Moreover, the expression of VprAP3 and VprPI might relate to glycolytic, fatty acid biosynthetic, and sucrose metabolic processes and co-expression with GAIP-B-like and YAB5. VprGI and other genes in the photoperiod pathway related to the circadian clock were co-expressed with some stress-responsive genes but probably downregulated the expression of VprAP3 and VprPI or VprUFO. Thus, we proposed an integrative model in which the transcription regulation of genes in the photoperiod pathway may coordinate the circadian clock, organ identity, and sugar–fatty acid/defense response for regulating the development of CH or CL in response to different photoperiods (Fig. 8), thus explaining the developmental evolution of dimorphic flowers.
Seeds of V. prionantha were collected and stored at the Northwest Normal University (Lanzhou, Gansu, China), and they are available upon request. The seedlings of V. prionantha were cultured according to a previous study . The plants were grown at 22–28 °C under 10-, 12-, or 16-h daylight. To further study the effect of the photoperiod on CH and CL flower development, plants with CL flowers under 16-h daylight were switched to 10-h daylight to continue culture, and plants with CH flowers under 10-h daylight were switched to 16-h daylight to continue culture. The temperature was maintained by air conditioning. The humidity was maintained at around 48%, and the light intensity was 116 μmol m−2 s−1. Plants under different daylight conditions were grown in parallel on different shelves. The daylight length was controlled by a time controller on each shelf.
The procedure of phenotypic analyses is similar to a previous description  without special note. Days to flower opening were counted from the beginning of every treatment under different photoperiods. The morphology of the flower buds was observed under a stereomicroscope (Olympus SZ61, Tokyo, Japan). The ratios of CH, inCL, and CL flowers were evaluated under 10-, 12-, and 16-h daylight. One hundred plants were observed in each photoperiod, and approximately 200 flower buds were counted in each case. In addition, after plants with CL flowers under 16-h daylight or CH flowers under 10-h daylight were switched to 10-h daylight or 16-h daylight, respectively, approximately 20 flower buds were observed under a stereomicroscope (Olympus SZ61, Tokyo, Japan) every 2, 4, 6, 8, and 10 days. The images were captured using a camera linked to a stereomicroscope (Olympus SZ61, Tokyo, Japan).
Iso-seq data analysis
The total RNA from the indicated tissues of V. prionantha was extracted using an Rneasy Plant Mini Kit (Qiagen, Dusseldorf, Germany), and was qualified and quantified using a Nano Drop and Agilent 2100 bioanalyzer (Thermo Fisher Scientific, Waltham, Massachusetts, USA). We sequenced two libraries of full-length transcripts using PacBio Iso-Seq (BGI, Shenzhen, China). Two samples from the whole plants with CH flowers and the whole plants with CL flowers of V. prionantha (including the roots, stems, leaves, and floral buds) were collected. The RNA extracted from the samples was mixed in equal amounts to obtain transcriptomes from various plant tissues and treatments. Approximately 20 µg of total RNA (400 ng/mL) was used to prepare the cDNA library. First strand cDNA was synthesized by Clontech SMARTer PCR cDNA Synthesis Kit (Clontech, Mountain View, California, USA). The CDS Primer IIA was first annealed to the polyA+ tail of transcripts, followed by first-strand synthesis with SMARTScribe™ Reverse Transcriptase (Clontech, Mountain View, California, USA). The raw reads were processed using SMRT Link 5.0 software (https://www.pacb.com/support/software-downloads/). We clustered and polished the full-length (FL) sequences using an isoform-level clustering algorithm, iterative clustering for error correction (ICE), and the Quiver tool in SMRT Link software. The FL reads were further corrected with RNA-seq reads using LoRDEC  with the parameters of ‘-k19 -s 3 -T 4’, and redundancy was removed using Cd-hit  with the parameters of ‘-c 0.99 -T 10 -G 0 -aL 0 -aS 0.99 -AS 30 -d 0 -p 1’.
RNA-seq data analysis
The total RNA was separately extracted and processed from three different development stages of floral buds, including the first development stage (S1), the third development stage (S3), and the fifth development stage (S5) of CH and CL flowers in V. prionantha using an Rneasy Plant Mini Kit (Qiagen, Dusseldorf, Germany). The polyA mRNAs were enriched using the magnetic oligo (dT) beads (NEB, Ipswich, Massachusetts, USA) and then were fragmented into 200 bp pieces. Next, random hexamer (N6) primers (Sangon Biotech, Shanghai, China) were used to build double strand cDNA libraries for all the samples. The cDNA libraries were constructed and sequenced using a BGISEQ-500 platform instrument (BGI, Shenzhen, China). The sequencing reads containing low-quality, adaptor-polluted, and high content of unknown bases (N) were removed before downstream analyses using Trimmomatic (V0.36)  with the parameters of ‘SE -phred33 ILLUMINACLIP: Trimmomatic-0.36/adapters/TruSeq3-SE. fa: 2:30:10 LEADING: 20 TRAILING: 20 SLIDINGWINDOW: 4:20 MINLEN: 50’.
Transcript functional annotation
Blast, Blast2GO, and InterProScan were used to perform functional annotation with transcripts. Unigenes were searched against five databases, including Cluster of Orthologous Groups of proteins (COG), SwissProt, NCBI non-redundant (NR), Gene Ontology (GO), and Kyoto Encyclopedia of Genes and Genomes (KEGG) (www.kegg.jp/kegg/kegg1.html). Functional annotation of unigenes was obtained from sequence similarity alignment using the BLAST algorithm with a criterion of E-value < 1e-10.
Gene family expansion and contraction analysis
To perform the gene family analysis, the amino acid sequences of V. prionantha and the relevant plant species (download from the NCBI database) were selected. We used OrthoFinder v2.4.1  to perform gene family clustering with the markov clustering (MCL) inflation parameter of 1.5. We constructed a phylogenetic tree for V. prionantha and the selected plants based on single-copy orthologous genes. Amino acid sequences were extracted from the sequences of each single-copy gene family and concatenated into a supergene for each species. Multiple sequence alignment was performed with MUSCLE v3.8.31 , followed by the construction of a phylogenetic species tree using maximum likelihood in RAxML v8.2.12 . Gene families were further filtered if one species had more than 200 genes. The remaining gene families were used to run CAFÉ (version4.1)  with default parameters.
Gene mapping and expression analysis
Initially, RNA-seq clean reads from 18 samples were mapped to the unique non-redundant isoforms obtained from the ISO-seq data and used as the “reference transcripts” because no reference genome was available for V. prionantha. We mapped all clean-read transcripts using HISAT (V2.1.0)  with the parameters of ‘–dta -p 10 -x -U’. Any unmapped, qc-failed and PCR duplicated reads were filtered out, and only the alignments with high-quality (MAPQ > = 10) were used for the downstream analysis. Based on the HISAT results, we calculated the gene expression level for each sample using StringTie (V1.3.3b) . The normalized expression levels of the resultant isoforms were estimated based on transcripts per million (TPM) as the expression of each transcript for downstream analysis. Then, we calculated Pearson’s correlation between all samples, performed hierarchical clustering between all samples using hclust, performed PCA analysis with all samples using princomp, and drew the diagrams with the ggplot2 function in R (https://sourceforge.net/projects/ggplot2.mirror/).
Detection of DEGs
The gene expression levels among the samples were examined based on RNA-seq data using the DEseq2 package  with default parameters. The high-quality total alignments were used in DEG detection. A P-adjust value < 0.05, and Log2 (fold change of Sample1/Sample2) for a gene > 1 or < − 1 were used as the screening cutoffs for determining extremely significant differential gene expression between paired samples.
Function enrichment analysis
The function of all genes collected was determined to elucidate the biological processes and pathways characterized in each developmental stage with R package clusterProfiler (v3.14) . We obtained the results of biological process (BP), cellular component (CC), and molecular function (MF). The reference background set was the GO terms of all genes, and a P-value < 0.01 was regarded as significant.
Identification and phylogenetic analysis of MADS-box genes
To identify MADS-box genes in V. prionantha, we firstly retrieved well-studied and annotated subtypes of MADS-box genes in A. thaliana, and then performed BLASTP analysis using these well-annotated A. thaliana MIKC-type MADS-box genes as queries, against the amino acid sequences in V. prionantha employing BLASTP (E-value < 10–5, and Identity score > 75). The identified putative MADS-box genes were further manually inspected using InterProScan (http://www.ebi.ac.uk/interpro/). To construct the phylogeny of these MADS-box genes, amino acid sequences were first aligned using MUSCLE v3.8.31 . The poorly aligned regions were removed using trimAL v3117  with a parameter of ‘-gt 0.9 -phylip’. A phylogenetic tree was constructed using maximum likelihood in RAxML v8.2.12  under the “GTRGAMMA” model with 100 bootstrap replicates.
Gene co-expression network analysis
We chose all DEGs to analyze gene co-expression network using the R package WGCNA (Weighted Correlation Network Analysis) Version: V1.48, and exactly followed the mannual protocol of this package . It is briefly described as follows. The power parameter was pre-calculated by the pickSoft Threshold function. It can provide the appropriate soft-thresholding power for network construction by calculating the scale-free topology fit index for several powers. Turning adjacency into topological overlap was carried out, which measured the network connectivity of a gene, and defined as the sum of its adjacency with all other genes for network generation. The hierarchical clustering function was used to classify genes with similar expression profiles into modules based on topological overlap matrix (TOM) dissimilarity, with a minimum size of 30 and a maximum size of 5000 for the gene dendrogram. The dissimilarity of MEs was calculated to choose a cutline to merge some modules.
Identification of significant modules and hub genes
Following the WGCNA pipeline , we calculated the correlation between MEs and traits (CH or CL flower) to identify the relevant modules. Next, gene significance (GS) was defined as the log10 transformation of the P-value in the linear regression between gene expression and trait information. In addition, module significance (MS) was defined as the average GS for all genes in a module. Each resulting model was visualized with Cytoscape software (http://www.cytoscape.org/). Key modules were selected and visualized using Cytoscape, and hub genes in networks were screened out using the Maximal Clique Centrality (MCC) score with the cytoHubba tool in Cytoscape (https://apps.cytoscape.org/apps/cytohubba) . Hub genes ranked in the top 20 module networks were chosen as candidates for further analysis and validation.
The procedure for qRT-PCR was described in a previous study . Briefly, gene expression was investigated using qRT-PCR in a Light-cycler480 (Roche, Mannheim, Germany) with an SYBR Premix Ex Taq Kit (Takara, Dalian, China) using gene-specific primers (Table S26). First-strand cDNA was synthesized from 2.0 μg of total RNA with oligo(dT) and M-MLV Reverse Transcriptase (Takara, Dalian, China). The expression of the endogenous 18S ribosomal RNA gene was used as an internal control . The amplification conditions were initial denaturation at 95 °C for 30 s, followed by 40 cycles of 95 °C for 5 s, and 60 °C for 30 s. Three independent biological samples were used. The relative expression level was evaluated according to a previous description .
Cloning and prediction of VprAP3 and VprPI promoters
Based on the CDS sequences of VprAP3 and VprPI, gDNA sequences were obtained using LA Taq (Takara, Dalian, China) with gene-specific primers (Table S26). According to the gDNA sequences, the promoter sequences were acquired using the Genome Walking Kit (Takara, Dalian, China). Cis-element prediction was analyzed by PlantCARE (http://bioinformatics.psb.ugent.be/webtools/plantcare/html/) and New PLACE (https://www.dna.affrc.go.jp/PLACE/?action=newplace).
The mean ± standard deviation was calculated from at least three independent replicates. Significance differences were analyzed by Duncan in SPASS13.0.
Availability of data and materials
All relevant supporting data can be found within the additional files accompanying this article. The promoter sequences of VprPI and VprAP3 reported in this article can be found in NCBI (http://www.ncbi.nlm.nih.gov) under the accession numbers ON125105 and ON125106. The raw RNA-seq data have been deposited in the NGDC in this article can be found in BIG Data Center (https://ngdc.cncb.ac.cn/) as a BioProject PRJCA008547.
Differentially expressed genes
Open reading frame
Real-time quantitative reverse transcription PCR
Principal component analysis
Kyoto encyclopedia of genes and genomes
Weighted correlation network analysis
Culley TM, Stokes RL. Genetic structure and outcrossing rates in Viola pedunculata (Violaceae), a California endemic Violet lacking cleistogamous flowers. Madroño. 2012;59:181–9.
Mayers AM, Lord EM. Comparative flower development in the cleistogamous species Viola odorata II An organographic study. Am J Bot. 1983;70:1556–63.
Culley TM, Klooster MR. The cleistogamous breeding system: a review of its frequency, evolution, and ecology in angiosperms. Bot Rev. 2007;73:1–30.
Lord EM. Cleistogamy: a tool for the study of floral morphogenesis, function and evolution. Bot Rev. 1981;47:421–49.
Minter TC, Lord EM. Effects of water stress, abscisic acid, and gibberellic acid on flower production and differentiation in the cleistogamous species Collomia grandiflora Dougl. ex Lindl. (Polemoniaceae). Am J Bot. 1983;70:618–24.
Campbell CS, Quinn JA, Cheplick GP, Bell TJ. Cleistogamy in grasses. Annu Rev Ecol Evol S. 1983;14:411–41.
Clavijo ERD, Jimenez MJ. Cleistogamy and chasmogamy in Ceratocapnos heterocarpa (Fumariaceae). Int J Plant Sci. 1993;154:325–33.
Wang Y, Ballard HE, McNally RR, Wyatt SE. Gibberellins are involved but not sufficient to trigger a shift between chasmogamous-cleistogamous flower types in Viola pubescens. J Torrey Bot Soc. 2013;140:1–8.
Li QX, Huo QD, Wang J, Zhao J, Sun K, He CY. Expression of B-class MADS-box genes in response to variations in photoperiod is associated with chasmogamous and cleistogamous flower development in Viola philippica. BMC Plant Biol. 2016;6:151.
Le Corff J. Effects of light and nutrient availability on chasmogamy and cleistogamy in an understory tropical herb, Calathea micans (Marantaceae). Am J Bot. 1993;80:1392–9.
Culley TM. Reproductive biology and delayed selfing in Viola pubescens (Violaceae), an understory herb with chasmogamous and cleistogamous flowers. Int J Plant Prod. 2002;163:113–22.
Koontz SM, Weekley CW, Crate SJH, Menges ES. Patterns of chasmogamy and cleistogamy, a mixed-mating strategy in an endangered perennial. AoB Plants. 2017;9:plx059.
Joly S, Schoen DJ. Repeated evolution of a reproductive polyphenism in plants is strongly associated with bilateral flower symmetry. Curr Biol. 2021;31:1515–20.
Stojanova B, Maurice S, Cheptou PO. Is plasticity across seasons adaptive in the annual cleistogamous plant Lamium amplexicaule? Ann Bot. 2016;117:681–91.
Ansaldi BH, Weber JJ, Goodwillie C, Franks SJ. Low levels of inbreeding depression and enhanced fitness in cleistogamous progeny in the annual plant Triodanis perfoliata. Botany. 2019;97:405–15.
Sternberger AL, Ruhil AVS, Rosenthal DM, Ballard HE, Wyatt SE. Environmental impact on the temporal production of chasmogamous and cleistogamous flowers in the mixed breeding system of Viola pubescens. PLoS ONE. 2020;15: e0229726.
Schemske DW. Evolution of reproductive characteristics in Impatiens (Balsaminaceae): the significance of cleistogamy and chasmogamy. Ecology. 1978;59:596–613.
Schoen DJ, Lloyd DG. The selection of cleistogamy and heteromorphic diaspores. Biol J Linn Soc. 1984;23:303–22.
Waller DM. Environmental determinants of outcrossing in Impatiens capensis (Balsaminaceae). Evolution. 1980;34:747–61.
Steets JA, Ashman TL. Herbivory alters the expression of a mixed-mating system. Am J Bot. 2004;91:1046–51.
Sternberger AL, Bowman MJ, Kruse CPS, Childs KL, Ballard HE, Wyatt SE. Transcriptomics identifies modules of differentially expressed genes and novel cyclotides in Viola pubescens. Front Plant Sci. 2019;10:156.
Miranda AS, Vieira MF. Production of floral morphs in cleistogamous Ruellia brevifolia (Pohl) C. Ezcurra (Acanthaceae) at different levels of water availability. J Pollinat Ecol. 2016;19:104–7.
Li QX, Li JG, Pan CC, Zhang L, Yang N, Sun K, He CY. Gibberellins is involved in the dimorphic flower development in Viola philippica. Plant Sci. 2021;303:110749.
Srikanth A, Schmid M. Regulation of flowering time: all roads lead to Rome. Cell Mol Life Sci. 2011;68:2013–37.
Andres F, Coupland G. The genetic basis of flowering responses to seasonal cues. Nat Rev Genet. 2012;13:627–39.
Irish VF, Sussex IM. Function of the apetala-1 gene during Arabidopsis floral development. Plant Cell. 1990;2:741–53.
Bowman JL, Smyth DR, Meyerowitz EM. Genetic interactions among floral homeotic genes of Arabidopsis. Development. 1991;112:1–20.
Bowman JL, Alvarez J, Weigel D, Meyerowitz EM, Smyth DR. Control of flower development in Arabidopsis thaliana by APETALA1 and interacting genes. Development. 1993;119:721–43.
Mandel MA, Gustafson-Brown C, Savidge B, Yanofsky MF. Molecular characterization of the Arabidopsis floral homeotic gene APETALA1. Nature. 1992;360:273–7.
Causier B, Schwarz-Sommer Z, Davies B. Floral organ identity: 20 years of ABCs. Semin Cell Dev Biol. 2010;21:73–9.
Irish VF. The flowering of Arabidopsis flower development. Plant J. 2010;61:1014–28.
Jack T, Brockman LL, Meyerowitz EM. The homeotic gene APETALA3 of Arabidopsis thaliana encodes a MADS box and is expressed in petals and stamens. Cell. 1992;68:683–97.
Goto K, Meyerowitz EM. Function and regulation of the Arabidopsis floral homeotic gene. PISTILLATA Genes Dev. 1994;8:1548–60.
Wuest SE, O’Maoileidigh DS, Rae L, Kwasniewska K, Raganelli A, Hanczaryk K, Lohan AJ, Loftus B, Graciet E, Wellmer F. Molecular basis for the specification of floral organs by APETALA3 and PISTILLATA. Proc Natl Acad Sci USA. 2012;109:13452–7.
Zhang SH, Zhang JS, Zhao J, He CY. Distinct subfunctionalization and neofunctionalization of the B-class MADS-box genes in Physalis floridana. Planta. 2015;241:387–402.
Lee OR. AmGAI-like interacts with ROSINA, a putative transcriptional regulator of DEFICIENS in Antirrhinum majus. Plant Sci. 2010;178:366–73.
Liao H, Fu X, Zhao H, Cheng J, Zhang R, Yao X, Duan X, Shan H, Kong H. The morphology, molecular development and ecological function of pseudonectaries on Nigella damascena (Ranunculaceae) petals. Nat Commun. 2020;11:1777.
Roth O, Alvarez JP, Levy M, Bowman JL, Ori N, Shani E. The KNOXI transcription factor SHOOT MERISTEMLESS regulates floral fate in Arabidopsis. Plant Cell. 2018;30:1309–21.
Lee I, Wolfe DS, Nilsson O, Weigel D. A LEAFY co-regulator encoded by UNUSUAL FLORAL ORGANS. Curr Biol. 1997;7:95–104.
Chae E, Tan QK, Hill TA, Irish VF. An Arabidopsis F-box protein acts as a transcriptional co-factor to regulate floral development. Development. 2008;135:1235–45.
Laufs P, Coen E, Kronenberger J, Traas J, Doonan J. Separable roles of UFO during floral development revealed by conditional restoration of gene function. Development. 2003;130:785–96.
Lee JY, Baum SF, Alvarez J, Patel A, Chitwood DH, Bowman JL. Activation of CRABS CLAW in the nectaries and carpels of Arabidopsis. Plant Cell. 2005;17:25–36.
Borghi M, Fernie AR. Floral metabolism of sugars and amino acids: implications for pollinators’ preferences and seed and fruit set. Plant Physiol. 2017;175:1510–24.
Millar AA, Clemens S, Zachgo S, Giblin EM, Taylor DC, Kunst L. CUT1, an Arabidopsis gene required for cuticular wax biosynthesis and pollen fertility, encodes a very-long-chain fatty acid condensing enzyme. Plant Cell. 1999;11:825–38.
Xiao C, Somerville C, Anderson CT. POLYGALACTURONASE involved in expension1 functions in cell elongation and flower development in Arabidopsis. Plant Cell. 2014;26:1018–35.
Ogawa M, Kay P, Wilson S, Swain SM. ARABIDOPSIS DEHISCENCE ZONE POLYGALACTURONASE1 (ADPG1), ADPG2, and QUARTET2 are polygalacturonases required for cell separation during reproductive development in Arabidopsis. Plant Cell. 2009;21:216–33.
Sampedro J, Pardo B, Gianzo C, Guitián E, Revilla G, Zarra I. Lack of a-xylosidase activity in Arabidopsis alters xyloglucan composition and results in growth defects. Plant Physiol. 2010;154:1105–15.
Dong X, Jiang Y, Hur Y. Genome-wide analysis of glycoside hydrolase family 1 β-glucosidase genes in Brassica rapa and their potential role in pollen development. Int J Mol Sci. 2019;20:1663.
Sawa M, Kay SA. GIGANTEA directly activates flowering locus T in Arabidopsis thaliana. Proc Natl Acad Sci USA. 2011;108:11698–703.
Sawa M, Nusinow DA, Kay SA, Imaizumi T. FKF1 and GIGANTEA complex formation is required for day-length measurement in Arabidopsis. Science. 2007;318:261–5.
Kinoshita A, Richter R. Genetic and molecular basis of floral induction in Arabidopsis thaliana. J Exp Bot. 2020;71:2490–504.
Lee J, Lee I. Regulation and function of SOC1, a flowering pathway integrator. J Exp Bot. 2010;61:2247–54.
Song YH, Smith RW, To BJ, Millar AJ, Imaizumi T. FKF1 conveys timing information for CONSTANS stabilization in photoperiodic flowering. Science. 2012;336:1045–9.
Wigge PA, Kim MC, Jaeger KE, Busch W, Schmid M, Lohmann JU, Weigel D. Integration of spatial and temporal information during floral induction in Arabidopsis. Science. 2005;309:1056–9.
Liu C, Xi W, Shen LS, Tan C, Yu H. Regulation of floral patterning by flowering time genes. Dev Cell. 2009;16:711–22.
Fudge JB, Lee RH, Laurie RE, Mysore KS, Wen J, Weller JL, Macknight RC. Medicago truncatula SOC1 genes are up-regulated by environmental cues that promote flowering. Front Plant Sci. 2018;9:496.
Balanzà V, Martínez-Fernández I, Ferrándiz C. Sequential action of FRUITFULL as a modulator of the activity of the floral regulators SVP and SOC1. J Exp Bot. 2014;65:1193–203.
Cheng H, Song S, Xiao L, Soo HM, Cheng Z, Xie D, Peng J. Gibberellin acts through jasmonate to control the expression of MYB21, MYB24, and MYB57 to promote stamen filament growth in Arabidopsis. PLoS Genet. 2009;5: e1000440.
Li Y, Qiu L, Liu X, Zhang Q, Zhuansun X, Fahima T, Krugman T, Sun Q, Xie C. glycerol-induced powdery mildew resistance in wheat by regulating plant fatty acid metabolism, plant hormones cross-talk, and pathogenesis related genes. Int J Mol Sci. 2020;21:673.
Liu W, Karemera NJU, Wu T, Yang Y, Zhang X, Xu X, Wang Y, Han Z. The ethylene response factor AtERF4 negatively regulates the iron deficiency response in Arabidopsis thaliana. PLoS ONE. 2017;12: e0186580.
Xu XD, Yuan L, Xie QG. The circadian clock ticks in plant stress responses. Stress Biology, 2022, 1–19, https://doi.org/10.1007/s44154-022-00040-7
Fornara F, de Montaigu A, Sánchez-Villarreal AS, Takahashi Y, van Themaat EVL, Huettel B, Davis SJ, Coupland G. The GI–CDF module of Arabidopsis affects freezing tolerance and growth as well as flowering. Plant J. 2015;81:695–706.
Baek D, Kim W, Cha J, Park HJ, Shin G, Park J, Lim CJ, Chun HJ, Li N, Kim DH, Lee SY, Pardo JM, Kim MC, Yun D. The GIGANTEA-ENHANCED EM LEVEL complex enhances drought tolerance via regulation of abscisic acid synthesis. Plant Physiol. 2020;184:443–58.
Lohmann JU, Weigel D. Building beauty: the genetic control of floral patterning. Dev Cell. 2002;2:135–42.
Lenhard M, Bonhert A, Jurgens G, Laux T. Termination of stem cell maintenance in Arabidopsis floral meristems by interactions between WUSCHEL and AGAMOUS. Cell. 2001;105:805–8.
Lohmann JU, Hong RL, Hobe M, Busch MA, Parcy F, Simon R, Weigel D. A molecular link between stem cell regulation and floral patterning in Arabidopsis. Cell. 2001;105:793–803.
Muhlemann JK, Klempien A, Dudareva N. Floral volatiles: from biosynthesis to function. Plant Cell Environ. 2014;37:1936–49.
Bolouri-Moghaddam MR, Roy KL, Xiang L, Rolland F, Van den Ende W. Sugar signalling and antioxidant network connections in plant cells. FEBS J. 2010;277:2022–37.
Van den Ende W. Multifunctional fructans and raffinose family oligosaccharides. Front Plant Sci. 2013;4:247.
Kebede A, Kebede M. In silico analysis of promoter region and regulatory elements of glucan endo-1,3-beta-glucosidase encoding genes in Solanum tuberosum: cultivar DM 1–3 516 R44. J Genet Eng Biotechnol. 2021;19:145.
Dotson BR, Soltan D, Schmidt J, Areskoug M, Rabe K, Swart C, Widell S, Rasmusson AG. The antibiotic peptaibol alamethicin from Trichoderma permeabilises Arabidopsis root apical meristem and epidermis but is antagonised by cellulase-induced resistance to alamethicin. BMC Plant Biol. 2018;18:165.
Salmela L, Rivals E. LoRDEC: accurate and efficient long read error correction. Bioinformatics. 2014;30:3506–14.
Li W, Godzik A. Cd-hit: a fast program for clustering and comparing large ets of protein or nucleotide sequences. Bioinformatics. 2006;22:1658–9.
Bolger AM, Lohse M, Usadel B. Trimmomatic: a flexible trimmer for Illumina sequence data. Bioinformatics. 2014;30:2114–20.
Emms DM, Kelly S. OrthoFinder: phylogenetic orthology inference for comparative genomics. Genome Biol. 2019;20:238.
Edgar RC. MUSCLE: multiple sequence alignment with high accuracy and high throughput. Nucleic Acids Res. 2004;32:1792–7.
Stamatakis A. RAxML version 8: a tool for phylogenetic analysis and post-analysis of large phylogenies. Bioinformatics. 2014;9:1312–3.
De Bie T, Cristianini N, Demuth JP, Hahn MW. CAFE: a computational tool for the study of gene family evolution. Bioinformatics. 2006;22:1269–71.
Kim D, Langmead B, Salzberg SL. HISAT: a fast spliced aligner with low memory requirements. Nat Methods. 2015;12:357–60.
Pertea M, Pertea G, Antonescu C, Chang T, Mendell JT, Salzberg SL. StringTie enables improved reconstruction of a transcriptome from RNA-seq reads. Nat Biotechnol. 2015;33:290–5.
Love MI, Huber W, Anders S. Moderated estimation of fold change and dispersion for RNA-seq data with DESeq2. Genome Biol. 2014;15:550.
Yu G, Wang L, Han Y, He Q. clusterProfiler: an R package for comparing biological themes among gene clusters. OMICS: J Plant Biol. 2012;16:284–7.
Capella-Gutiérrez S, Silla-Martínez JM, Gabaldón T. trimAl: a tool for automated alignment trimming in large-scale phylogenetic analyses. Bioinformatics. 2009;25:1972–3.
Langfelder P, Horvath S. WGCNA: an R package for weighted correlation network analysis. BMC Bioinformatics. 2008;9:559.
Chin CH, Chen SH, Wu HH, Ho CW, Ko MT, Lin CY. cytoHubba: identifying hub objects and sub-networks from complex interactome. BMC Syst Biol. 2014;8:S11.
Livak KJ, Schmittgen TD. Analysis of relative gene expression data using real-time quantitative PCR and the 2–△△CT method. Methods. 2001;25:402–8.
We sincerely thank the assistance of Dr. Lingyun Jia (Life Science College, Northwest Normal University) in qRT-PCR.
This work was supported by the grants (32160055, 31930007, and 31800188) from the National Natural Science Foundation of China, and the grant (21JR7RA140) from the Natural Science Foundation of Gansu province.
Ethics approval and consent to participate
Seeds of V. prionantha were permitted to collect at the Northwest Normal University (Lanzhou, Gansu, China), and they are available upon request. The identity of V. prionantha was identified by Professor Dr. Kun Sun (Northwest Normal University, Lanzhou, Gansu, China). All methods were performed in accordance with the relevant guidelines and regulations.
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Li, Q., Li, K., Zhang, Z. et al. Transcriptomic comparison sheds new light on regulatory networks for dimorphic flower development in response to photoperiod in Viola prionantha. BMC Plant Biol 22, 336 (2022). https://doi.org/10.1186/s12870-022-03732-4