- Research article
- Open Access
LATE ELONGATED HYPOCOTYL regulates photoperiodic flowering via the circadian clock in Arabidopsis
BMC Plant Biology volume 16, Article number: 114 (2016)
Plants constantly monitor changes in photoperiod or day length to trigger the flowering cycle at the most appropriate time of the year. It is well established that photoperiodic flowering is intimately associated with the circadian clock in Arabidopsis. In support of this notion, many clock-defective mutants exhibit altered photoperiodic sensitivity in inducing flowering. LATE ELONGATED HYPOCOTYL (LHY) and its functional paralogue CIRCADIAN CLOCK ASSOCIATED 1 (CCA1) constitute the core of the circadian clock together with TIMING OF CAB EXPRSSION 1 (TOC1). While it is known that TOC1 contributes to the timing of flowering entirely by modulating the clock function, molecular mechanisms by which LHY and CCA1 regulate flowering time have not been explored.
We investigated how LHY and CCA1 regulate photoperiodic flowering through molecular genetic and biochemical studies. It was found that LHY-defective mutants (lhy-7 and lhy-20) exhibit accelerated flowering under both long days (LDs) and short days (SDs). Consistent with the accelerated flowering phenotypes, gene expression analysis revealed that expression of the floral integrator FLOWERING LOCUS T (FT) is up-regulated in the lhy mutants. In addition, the expression peaks of GIGANTEA (GI) and FLAVIN-BINDING, KELCH REPEAT, F-BOX PROTEIN 1 (FKF1) genes, which constitute the clock output pathway that is linked with photoperiodic flowering, were advanced by approximately 4 h in the mutants. Furthermore, the up-regulation of FT disappeared when the endogenous circadian period is matched to the external light/dark cycles in the lhy-7 mutant. Notably, whereas CCA1 binds strongly to FT gene promoter, LHY does not show such DNA-binding activity.
Our data indicate that the advanced expression phases of photoperiodic flowering genes are associated with the clock defects in the lhy mutants and responsible for the reduced photoperiodic sensitivity of the mutant flowering, demonstrating that LHY regulates photoperiodic flowering via the circadian clock, similar to what has been shown with TOC1. It is notable that while LHY regulates photoperiodic flowering in a similar manner as with TOC1, the underlying molecular mechanism would be somewhat distinct from that exerted by CCA1 in Arabidopsis.
The appropriate timing of flowering is critical for reproductive success in plants. Since the transition from the vegetative to the reproductive phases is irreversible, plants precisely coordinate endogenous developmental signals and environmental cues, such as changes in photoperiod, light quality and quantity, and temperature, to optimize the timing of flowering [1–3]. Both the endogenous and environmental signals are incorporated into flowering genetic pathways via the floral integrators, such as FLOWERING LOCUS T (FT) and SUPPRESSOR OF CONSTANS OVEREXPRESSION 1 (SOC1) [4, 5].
Photoperiod is a major environmental cue that profoundly affects floral induction [2, 3, 6]. Plants monitor photoperiodic changes to anticipate seasonal changes. CONSTANS (CO), which is a B-box zinc finger transcription factor , plays a central role in photoperiodic flowering by activating FT expression [8, 9]. Accordingly, CO-defective mutants and CO-overexpressing plants exhibit photoperiod-insensitive flowering phenotypes [10, 11].
The photoperiod-sensitive FT induction is mediated by the distinct accumulation peak of CO in late afternoon under long days (LDs), which is shaped by the coordinated actions of several ubiquitin/proteasome-dependent pathways . A small group of E3 ubiquitin ligases and photoreceptors modulate the CO stability. The light signaling mediator CONSTITUTIVE PHOTOMORPHOGENIC 1 (COP1) degrades CO at night [13, 14]. In the light phase of the day, two opposing regulations occur through the actions of HIGH EXPRESSION OF OSMOTICALLY RESPONSIVE GENES 1 (HOS1) and FLAVIN-BINDING, KELCH REPEAT, F-BOX 1 (FKF1) E3 ubiquitin ligases. HOS1 degrades CO in the morning, and FKF1 stabilizes CO in late afternoon [15, 16]. The sequential actions of HOS1 and FKF1 contribute to the maintenance of CO accumulation at a basal level in the morning but at a high level in later afternoon, and thus Arabidopsis flowering is induced only under LDs . Meanwhile, PHYTOCHROME B mediates CO degradation, but PHYTOCHROME A and CRYTOCHROME photoreceptors mediate CO stabilization . It is notable that CO accumulation occurs at the specific time phase of the day under LDs, necessitating that photoperiodic flowering would be closely linked with the circadian clock [2, 3, 17].
Many clock-defective Arabidopsis mutants exhibit alterations in the photoperiodic sensitivity of flowering time, supporting the intimate linkage between the clock and photoperiodic flowering [18–22]. In addition, the circadian clock regulates the rhythmic expression of photoperiodic flowering genes, such as CO, FKF1, GIGANTEA (GI), and CYCLING DOF FACTOR 1 (CDF1) [23–26]. The clock allows the high-level expression of CO gene occurs in the light only under LDs . The clock-controlled peak of FKF1 and GI expression in the LD afternoon renders FKF1-GI complex to be formed, which is crucial for CO accumulation . On the other hand, the prevention of CO and FT expression by CDFs occurs in the morning through the clock function [26, 27]. It has been shown that the early flowering phenotypes of short-period plants, such as TIMING OF CAB EXPRESSION 1 (TOC1)-defective mutant (toc1) and CASEIN KINASE II BETA SUBUNIT 4 (CKB4)-overexpressing plants, are caused by the advanced expression peaks of photoperiodic flowering genes [28, 29].
While the altered flowering phenotypes of toc1 mutant and CKB4-overexpressing plants are entirely caused by clock defects, clock-independent control of photoperiodic flowering by clock components has also been proposed [30–32]. For instance, GI, which plays a role in regulating clock progression , activates FT expression by directly binding to its gene promoter independent of CO . It has recently been reported that SENSITIVITY TO RED LIGHT REDUCED 1 (SRR1), which is required for normal oscillator function , regulates floral transition in a CO-independent manner . Similarly, DE-ETIOLATED 1 (DET1), which is a transcriptional corepressor important for clock progression, acts as a floral repressor . It is notable that GI, SRR1, and DET1 regulate flowering time independent of their roles in the clock function. In addition, they do not require CO, the central promoter of photoperiodic flowering.
LATE ELONGATED HYPOCOTYL (LHY) and its functional paralogue CIRCADIAN CLOCK ASSOCIATED 1 (CCA1) constitute the central oscillator in Arabidopsis [20, 35, 36]. Arabidopsis mutants that are defective in LHY and CCA1 exhibit early flowering even under non-inductive conditions [20, 22, 37]. It has been shown that CCA1 regulates flowering time by binding to the SOC1 gene promoter . However, it has not been explored at the molecular level how LHY regulates flowering time.
In this work, with an aim of clarifying the molecular mechanism by which LHY regulates flowering time, we performed molecular genetic and biochemical studies on LHY-defective mutants (lhy-7 and lhy-20). Notably, the expression peaks of photoperiodic flowering genes were shifted earlier in the lhy mutants. We found that the advanced expression phases of photoperiodic flowering genes are associated with the clock defects in the mutants and underlie the reduced photoperiodic sensitivity of the mutant flowering. By matching the external light/dark cycles to the endogenous circadian period, the early flowering phenotype of the mutants was rescued. Interestingly, CCA1 binds strongly to the FT gene promoter, but LHY does not exhibit such DNA-binding activity. Our data indicate that while LHY regulates the timing of flowering entirely via the circadian clock like TOC1, CCA1 would be functionally distinct from TOC1 and LHY in regulating photoperiodic flowering.
Loss-of-function lhy mutants exhibit early flowering under both LDs and SDs
To investigate the functional roles of LHY in photoperiodic flowering, we examined the flowering phenotypes of LHY-defective mutants. We also aimed to clarify the molecular mechanisms by which LHY regulates flowering time: whether LHY affects flowering time entirely by modulating the circadian rhythms like TOC1  or regulating the expression of specific flowering genes like GI  or both. In additional to the previously reported lhy-20 mutant , we also isolated a T-DNA insertional loss-of-function mutant, which was designated lhy-7 (Fig. 1a). The lhy-7 mutant contains a single copy of T-DNA insertion in the sixth exon of LHY gene. Gene expression analysis confirmed lack of LHY transcription in the lhy-7 mutant (Fig. 1b).
It has been reported that the loss-of-function lhy-20 mutant exhibit a shortening of the circadian period [39, 40]. We investigated the circadian period of the lhy-7 mutant by examining the rhythmic expression patterns of two representative clock output genes, COLD, CIRCADIAN RHYTHM, AND RNA BINDING 2 (CCR2) and CHLOROPHYLL A/B-BINDING PROTEIN 2 (CAB2) [41, 42]. We found that the lhy-7 mutant also exhibits advanced peak expressions of the CCR2 and CAB2 genes compared to those observed in Col-0 plants (Additional file 1), as has been observed with other LHY-defective mutants [20, 37, 39, 40].
We next examined the flowering phenotypes of the lhy-7 and lhy-20 mutants under different daylengths by counting the number of rosette leaves at bolting. Both the lhy mutants showed accelerated flowering under LDs (Fig. 1c). The early flowering phenotypes of the mutants were more prominent under SDs (Fig. 1d). The reduced photoperiodic sensitivity of the lhy flowering is similar to what has been observed with LHY-defective mutants in other ecotypes [20, 37], showing that the altered flowering phenotypes are associated with LHY function. Since the flowering phenotypes of the lhy-7 and lhy-20 mutants were similar each other, we chose the former for subsequent molecular assays.
Expression patterns of flowering genes are altered in lhy-7 mutant
To obtain insights into the molecular mechanism by which LHY regulates flowering time, we analyzed the expression patterns of flowering genes under LDs and SDs. In LD-grown plants, the expression of FT and SOC1 genes was slightly but detectably elevated in the lhy-7 mutant (Fig. 2a), which is in good agreement with the flowering phenotype of the mutant. Under SDs, the expression of FT gene, but not SOC1 gene, was markedly elevated in the lhy-7 mutant (Fig. 2b), indicating that the FT induction is the major cause of the early flowering of the mutant at least under SDs.
It is known that the circadian clock is closely associated with photoperiodic flowering [1, 17, 37]. We therefore examined the expression patterns of photoperiodic flowering genes, such as CO, GI, and FKF1, in the lhy-7 mutant. The amplitude and waveform of CO transcription were not discernibly altered in the lhy-7 mutant under both LDs and SDs (Fig. 2a and b). In contrast, the waveforms of GI and FKF1 transcription appeared with advanced shifts of the peaks in the lhy-7 mutant under both photoperiod regimes. Considering that GI interacts with FKF1 to stabilize CO , it seems that the advanced expression phases of GI and FKF1 under SDs would lead to an elevation of the GI-FKF1 complex formation and stabilize CO, underscoring the FT induction and early flowering in the lhy-7 mutant.
We also investigated the expression patterns of flowering genes that belong to other flowering pathways, such as autonomous, thermosensory, and gibberellic acid (GA) pathways, under LDs and SDs. It was found that the expression patterns of autonomous pathway genes, such as FLOWERING LOCUS KH DOMAIN (FLK), FVE, and FCAγ, and GA pathway genes, such as SPYNDLY (SPY) and REPRESSOR OF GA1 (RGA1), were not altered in the lhy-7 mutant under both light regimes (Additional file 2). In addition, the transcription of two floral repressor genes, which play a role in temperature-responsive flowering, was not significantly affected in the mutant. While the transcript level of SHORT VEGETATIVE PHASE (SVP) gene in the mutant was comparable to that in Col-0 plants, the transcription of FLOWERING LOCUS M β (FLMβ) gene was marginally induced in the mutant (Additional file 2). Considering the floral repressive activity of FLMβ , it is apparent that the early flowering phenotype of the lhy-7 mutant is not associated with the slight induction of FLMβ gene.
FLC gene is not related with lhy-7 flowering
It has been reported that induction of the floral repressor FLOWERING LOCUS C (FLC) is linked with the late flowering phenotype of cca1 lhy double mutant grown under continuous light conditions . The FLC gene is also up-regulated in the parental lhy mutant in Landsberg erecta (Ler) background. We found that FLC expression is slightly increased in the lhy-7 mutant under LDs (Fig. 2a). In contrast, the FLC expression was not discernibly elevated in the mutant under SDs (Fig. 2b), suggesting that FLC gene is not associated with the mutant flowering phenotype.
To further examine whether FLC gene is associated with the flowering phenotype of the lhy-7 mutant, we crossed the lhy-7 mutant with the FLC-defective flc-3 mutant that exhibits early flowering, more prominently under SDs . We compared the flowering time of the resultant lhy-7 flc-3 double mutant with those of the parental mutants. The flowering phenotype of the lhy-7 flc-3 double mutant was not discernibly different from those of the single mutants under LDs (Fig. 3a). In contrast, the lhy-7 flc-3 double mutant flowered earlier than the single mutants under SDs (Fig. 3b), indicating that FLC gene is not directly associated with the flowering phenotype of the lhy-7 mutant.
LHY does not bind to FT promoter
LHY and CCA1 regulate a variety of genes by directly binding to the gene promoters [35, 38, 46]. For example, the CCA1 transcription factor represses SOC1 expression by binding directly to the gene promoter . We found that FT gene is significantly up-regulated in the lhy-7 mutant (Fig. 2). It was therefore suspected that LHY might repress FT expression perhaps by binding to the gene promoter.
Nucleotide sequence analysis identified a putative CCA1-binding sequence (CBS) in the FT gene promoter and a potential evening element (EE) in the first intron (Fig. 4a). To examine whether LHY binds to the CBS and EE sequences, we employed chromatin immunoprecipitation (ChIP) assays using transgenic plants overexpressing a LHY-MYC gene fusion, in which a MYC-coding sequence was fused in-frame to the 3′ end of the LHY-coding sequence (Additional file 3). We also included the transgenic plants overexpressing a MYC-CCA1 gene fusion in the assays. Both the 35S:LHY-MYC and 35:MYC-CCA1 transgenic exhibited elongated hypocotyls, disruption of circadian rhythms, and suppression of FT expression (Additional file 4), as reported previously [19, 47], confirming that the transgenic plants are relevant for ChIP assays. Quantitative ChIP-PCR runs revealed that CCA1 binds to the CBS and EE sequence elements (Fig. 4b). In contrast, LHY did not bind to the sequence elements, while it efficiently bound to the TOC1 gene promoter containing EE .
To verify the binding of CCA1 to FT chromatin, we performed electrophoretic mobility shift assay (EMSA) using a recombinant maltose binding protein (MBP)-CCA1 fusion protein. Consistent with the ChIP data, it was found that CCA1 binds specifically to CBS and EE sequence elements (Additional files 5 and 6).
To examine whether CCA1 binding to FT chromatin influences FT expression, we performed transient β-glucuronidase (GUS) expression assays by coexpressing the FT promoter-driven GUS reporter plasmid (FT pro:GUS) and the effector plasmids (35S:CCA1 or 35S:LHY) in Arabidopsis protoplasts. The assays showed that CCA1 negatively regulates GUS expression, but LHY does not affect GUS expression (Fig. 4c), consistent with the ChIP data. The repressive effects of CCA1 on GUS expression disappeared when a reporter plasmid harboring mutations in CBS was coexpressed, indicating that the binding of CCA1 to CBS is essential for the CCA1-mediated repression of FT expression. These observations indicate that although LHY and CCA1 are known to be functionally redundant [20, 48], LHY is distinct from CCA1 in regulating FT expression.
It has been reported that GI is associated with the flowering phenotype of cca1 lhy double mutant . While CCA1 is directly associated with GI promoter [38, 49], it is unknown whether LHY binds to GI promoter. ChIP assays using transgenic plants overexpressing a LHY-MYC gene fusion showed that LHY also binds to GI promoter (Additional file 7), like CCA1. Binding of both LHY and CCA1 to GI promoter is in harmony with the repression of GI expression in both CCA1- and LHY-inducible lines .
Clock defects underlie the reduced photoperiodic sensitivity of lhy flowering
LHY is a key component of the central oscillator of plant circadian clock. LHY-defective mutants exhibit a shortened circadian rhythm of approximately 20 h compared to that of Col-0 plants (, this work). We found that lhy-7 mutant exhibits early flowering with a reduced sensitivity to photoperiod. Therefore, a critical question was whether the reduced photoperiodic sensitivity of the lhy-7 flowering is interconnected with the clock defects in the mutant.
To address the question, we measured the flowering times of lhy-7 and lhy-20 mutants under light/dark (L/D) cycles that were matched to the endogenous circadian periods of the mutants. If the altered flowering times of the lhy mutants are entirely due to the clock defects, the flowering times would be restored by matching the external L/D cycles to the endogenous circadian period, as has been observed with TOC1-defective mutants [21, 28]. As expected, we found that the early flowering of the lhy mutants was completely annulled under SDs of 20 h (6.7 L: 13.3D) (Fig. 5a), which matches to the endogenous period of the mutants (, this work), indicating that LHY regulates flowering time entirely via the circadian clock.
We also analyzed the expression profiles of flowering time genes in the lhy-7 mutant under SDs of adjusted L/D cycles. The elevation of FT transcript levels was not observed when the lhy-7 mutant was grown under SDs of 20 h (Fig. 5b and Additional file 8), as has been observed with short-period plants, such as toc1 null mutants [28, 29]. It is therefore evident that the reduced photoperiod sensitivity of the lhy-7 flowering is caused by the clock defects.
It was found that CO transcription was elevated at night under the assay conditions (Fig. 5b). Since CO protein is degraded under dark conditions [13, 14], it is unlikely that the CO induction at night is physiologically important for the flowering phenotype of the lhy-7 mutant. The waveform of GI transcription under the adjusted L/D cycles was comparable to that in Col-0 plants under SDs of 24 h. In addition, gene expression assays revealed that the expression of flowering genes, such as FLK, FVE, FCAγ, SVP, SPY, and RGA1, was not altered in the lhy-7 mutant under both SDs of 20 and 24 h. The slight induction of FLMβ gene in the lhy-7 mutant under SDs of 24 h was also observed under SDs of 20 h (Additional files 2 and 9). On the basis of the flowering times and expression patterns of flowering genes in the lhy mutants under adjusted L/D cycles, we concluded that LHY regulates photoperiodic flowering via the clock function.
To verify that LHY regulates flowering time through the clock-controlled CO-FT pathway, we generated lhy-7 co-101 double mutant by crossing the lhy-7 mutant with the CO-defective co-101 mutant. Acceleration of flowering by the lhy mutation completely disappeared in the lhy-7 co-101 double mutant under LDs (Fig. 5c). Accordingly, FT expression was slightly induced in the lhy-7 mutant, but the induction was compromised in the lhy-7 co-101 double mutant (Fig. 5d). We also examined the level of FT transcripts in the single and double mutants under SDs, since the early flowering phenotype of the single mutant was more prominent under this light regime (Fig. 1d). We found that the elevation of FT expression in the lhy-7 mutant was completely annulled in the lhy-7 co-101 double mutant (Fig. 5d). Together, these observations indicate that LHY-mediated regulation of photoperiodic flowering depends on CO function.
LHY-mediated clock control of photoperiodic flowering
Plants sense photoperiodic changes by integrating light signals perceived by the photoreceptors and timing information provided by the circadian clock. In Arabidopsis, photoperiod-sensitive induction of the floral integrator FT is a crucial molecular event in photoperiodic flowering . It is known that the coordinated action of light signals and timing information allows the CO transcription factor to accumulate specifically in late afternoon under LDs, which is a prerequisite for the LD-specific induction of FT gene [1–3, 12]. The circadian clock regulates CO activity at both the transcriptional and posttranscriptional levels [12, 16, 23]. At the transcriptional level, the clock shapes the rhythmic expression patterns of CO in a way that a high level of CO transcripts accumulates during the light phase under LDs . At the posttranscriptional level, the circadian clock contributes to the stabilization of CO in late afternoon under LDs by modulating the expression of GI and FKF1 genes [16, 17].
In this study, we demonstrated that LHY, which is a core component of the central oscillator in Arabidopsis, regulates photoperiodic flowering by adjusting the rhythmic expression patterns of photoperiodic flowering genes, such as GI and FKF1. We found that the expression peaks of GI and FKF1 genes are shifted earlier in the lhy-7 mutant, which is consistent with the shortened circadian period of the mutant. A plausible explanation is that the advanced phases of GI and FKF1 expression in the lhy-7 mutant would lead to an increase in the formation of GI-FKF1 complexes during the light phase, resulting in a higher-level accumulation of CO in the mutant. In support of this view, the early flowering phenotype of the mutant was completely annulled by matching the external L/D cycles to the endogenous circadian period. Under these assay conditions, the phase shift of GI transcription was restored and the up-regulated expression of FT was suppressed to a basal level in the lhy-7 mutant. Together with the previous reports on short-period plants [28, 29], it seems that the circadian clock components, including LHY, regulates photoperiodic flowering by adjusting the expression timing of photoperiodic flowering genes.
Common and distinct roles of LHY and CCA1 in photoperiodic flowering
LHY and CCA1 are MYB motif-containing transcription factors that function at least in part redundantly in the circadian clock [19, 20, 48]. Whereas the gain-of-function mutations of both LHY and CCA1 genes disrupt circadian rhythms [19, 20], both the LHY- and CCA1-defective mutants exhibit shortened circadian periods [20, 37, 51]. The cca1 lhy double mutants show shorter circadian periods than the cca1 or lhy single mutants [20, 37, 48].
On the other hand, there have been some reports supporting distinct roles of CCA1 and LHY. For instance, LHY overexpression does not enhance pathogen resistance, whereas CCA1 overexpression induces pathogen resistance [52, 53]. Another example is the differential regulation of CCA1 and LHY expression by CCA1 HIKING EXPEDITION (CHE) and BROTHER OF LUX ARRHYTHMON (BOA), the components of the Arabidopsis circadian clock. While CHE and BOA bind directly to CCA1 gene promoter, they are not associated with LHY gene promoter [46, 54].
We found that CCA1, but not LHY, binds to FT gene promoter to repress its expression. It has been reported that CCA1 represses SOC1 expression by binding to the gene promoter . We observed that SOC1 expression is not discernibly affected by lhy mutations, suggesting that LHY is not related with SOC1 expression. It is known that LHY and CCA1 form both homodimers and heterodimers in vivo [47, 55]. One possibility is that whereas common roles of the two transcription factors would be related with the LHY-CCA1 heterodimers, their distinct roles would be exerted through the homodimers.
Clock-independent control of photoperiodic flowering
It is now apparent that most clock components, including LHY, TOC1, and CKB4, regulate photoperiodic flowering via the clock function [28, 29]. Notably, the shorter the circadian periods of clock mutants, the earlier the flowering times of the mutants in most cases , supporting that the clock regulates photoperiodic flowering by modulating the rhythmic expression of photoperiodic flowering genes [1, 6, 17].
However, there are recent reports supporting that some clock components affect flowering time through clock-independent pathways. CCA1 regulates the expression of floral integrators by directly binding to the gene promoters (, this work). GI also binds directly to FT gene promoter . In addition, the early flowering phenotype of DET1-defective mutants is not restored by matching the external L/D cycles to the endogenous circadian period of the mutants, indicating that DET1 negatively regulates flowering independent of its role in the clock function . Together, it is likely that clock components regulate photoperiodic flowering through both CO-mediated, clock-dependent and CO-free, clock-independent pathways. It will be interesting to investigate how individual clock components regulate flowering time and how the clock-dependent and clock-independent pathways are functionally inter-connected with each other in photoperiodic flowering.
We investigated how LHY regulates photoperiodic flowering by performing molecular genetic and biochemical studies. LHY regulates photoperiodic flowering entirely via the circadian clock. In the LHY-defective mutants, the early flowering phenotypes and the shifted phases of photoperiodic flowering gene expression were recovered by matching the external L/D cycles to the endogenous circadian periods of the mutants. It is notable that the mechanism by which LHY regulates photoperiodic flowering is somewhat distinct from that exerted by CCA1. Our findings would contribute to better understanding of how the clock function is associated with flowering time control in response to photoperiodic signals.
Plant genotypes and growth conditions
Arabidopsis thaliana lines used were in the Columbia (Col-0) background, unless specified otherwise. Arabidopsis plants were grown either in soil or on 1/2 X Murashige and Skoog (MS)-agar plates (hereafter referred to as MS-agar plates) at 23 °C under either LDs (16-h light and 8-h dark) or SDs of 24 h (8 L: 16D) or 20 h (6.7 L: 13.3D) total duration. White light illumination (120 μmol photons m−2s−1) was provided by fluorescent FLR40D/A tubes (Osram, Seoul, Korea).
T-DNA insertional gene knockout mutants lhy-20, flc-3, and co-101 have been described previously [39, 45, 56]. The LHY-deficient lhy-7 mutant (SALK-149287) was isolated from a T-DNA insertional mutant pool deposited in the Arabidopsis Information Resource (TAIR, Ohio State University, OH). Homozygotic lines were obtained by selection for three or more generations and analysis of segregation ratios. Lack of gene expression in the mutants was verified by RT-PCR before use.
A MYC-coding sequence was fused in-frame to the 5′ end of the CCA1-coding sequence or to the 3′ end of the LHY-coding sequence, and the gene fusions were subcloned into the pBA002 vector under the control of the Cauliflower Mosaic Virus (CaMV) 35S promoter. The expression constructs were transformed into Col-0 plants, resulting in 35S:MYC-CCA1 and 35S:LHY-MYC, respectively. Overexpression of the transgenes was verified by quantitative real-time RT-PCR (qRT-PCR).
Gene expression assay
Extraction of total RNA samples from appropriate plant materials and qRT-PCR conditions have been described previously . Total RNA samples were pretreated with RNase-free DNase to eliminate contaminating genomic DNA before use.
RNA sample preparation, reverse transcription, and quantitative PCR were conducted according to the criteria that have been proposed to ensure reproducible and accurate measurements .
qRT-PCR reactions were performed in 96-well blocks with an Applied Biosystems 7500 Real-Time PCR System (Foster City, CA) using the SYBR Green I master mix in a reaction volume of 20 μl. The PCR primers were designed using the Primer Express Software installed in the system and listed in Additional file 10. The two-step thermal cycling profile employed was 15 s at 94 °C and 1 min at 68 °C. An eIF4A gene (At3g13920) was included in the reactions as internal control to normalize the variations in the amounts of cDNA used. All the qRT-PCR reactions were performed in biological triplicates using RNA samples extracted from three independent plant materials grown under identical conditions. The comparative ΔΔCT method was employed to evaluate relative quantities of each amplified product in the samples. The threshold cycle (CT) was automatically determined for each reaction using the default parameters of the system. The specificity of PCR reactions was determined by melt curve analysis of the amplified products using the standard method installed in the system.
ChIP assays were performed, essentially as described previously , in biological triplicates using three independent plant materials grown under identical conditions. Seven-day-old 35S:MYC-CCA1 and 35S:LHY-MYC transgenic plants grown on MS-agar plates were vacuum-infiltrated with 1 % (v/v) formaldehyde for cross-linking and ground in liquid nitrogen after quenching the cross-linking process. Chromatin preparations were sonicated into 0.5- to 1-kb fragments. An anti-MYC antibody (Millipore, Billerica, MA) was added to the chromatin solution, which was precleared with salmon sperm DNA/protein G agarose beads (Roche, Indianapolis, IN). The precipitates were eluted from the beads. Cross-links were reversed, and residual proteins were removed by incubation with proteinase K. DNA was recovered using the QIAquick PCR purification kit (Qiagen, Valencia, CA). Quantitative PCR was performed to determine the amounts of genomic DNA enriched in the chromatin preparations. The primers used are listed in Additional file 10.
Transient expression assays in Arabidopsis protoplasts
In the reporter vector, a 2-kb promoter sequence of FT gene was transcriptionally fused to the β-glucuronidase (GUS) gene. The GUS reporter construct harboring a mutated CCA1-binding sequence (CBS) within the FT promoter was used to investigate the effects of CBS on the binding of CCA1 and LHY to the FT promoter. The CCA1- and LHY-coding sequences were subcloned under the control of the CaMV 35S promoter in the effector vector. The reporter and effector vectors were cotransfected into Arabidopsis mesophyll protoplasts by the polyethylene glycol (PEG)-calcium transfection method . The CaMV 35S promoter-luciferase construct was also cotransfected as internal control. GUS activity was measured by a fluorometric method as described previously . Luciferase activity assay was performed using the Luciferase Assay System kit (Promega, Madison, WI). GUS activities were normalized by luciferase activities.
Flowering time measurement
Plants were grown in soil at 23 °C under either long days of 24 h or short days of 24 h (8 L: 16D) or 20 h (6.6 L: 13.4D) total duration until flowering. Numbers of rosette leaves at bolting were counted, and 20 countings were averaged for each measurement.
Circadian rhythm measurement
Plants were entrained to long day cycles and then transferred to continuous light conditions for 3 days. To trace the circadian rhythm, whole plant materials were harvested at appropriate zeitgeber time (ZT) points for total RNA extraction. Gene transcript levels were measured by qRT-PCR.
Preparation of recombinant MBP-CCA1 fusion protein
A CCA1-coding sequence was subcloned into the pMAL-c2X Escherichia coli (E. coli) expression vector (NEB, Ipswich, MA) harboring a maltose binding protein (MBP)-coding sequence. Recombinant MBP-CCA1 fusion protein was produced in E. coli Rosetta2 (DE3) pLysS strain (Novagen, Madison, WI). Harvested cells were resuspended in MBP buffer (20 mM Tris-HCl, pH 7.4, 200 mM NaCl, 1 mM EDTA, 10 mM 2-mercaptoethanol, 1 mM PMSF, and protease inhibitor cocktail (Roche, Indianapolis, IN)). Cell lysates were prepared by running three cycles of freezing and thawing followed by centrifugation. The fusion proteins were affinity-purified as described previously .
EMSA was performed using recombinant MBP-CCA1 fusion protein, as described previously . DNA fragments were end-labeled with γ-32P[dATP] using T4 polynucleotide kinase (Takara, Kyoto, Japan). Labeled probes were incubated with 100 ng of MBP or MBP-CCA1 fusion protein for 30 min at room temperature in binding buffer (10 mM Tris-HCl, pH 7.6, 50 mM NaCl, 1 mM EDTA, 5 mM DTT, 5 % glycerol) supplemented with 100 ng poly(dI-dC) in the presence or absence of competitor DNA fragments. The reaction mixtures were resolved on 6 % non-denaturing polyacrylamide gel at 100 V for 1 h. The gels were dried on Whatman 3 MM paper and exposed to X-ray film.
BROTHER OF LUX ARRHYTHMO
CHLOROPHYLL A/B-BINDING PROTEIN 2
CIRCADIAN CLOCK ASSOCIATED 1
COLD, CIRCADIAN RHYTHM, AND RNA BINDING 2
CYCLING DOF FACTOR 1
CCA1 HIKING EXPEDITION
CASEIN KINASE II BETA SUBUNIT 4
CONSTITUTIVE PHOTOMORPHOGENIC 1
electrophoretic mobility shift assay
FLAVIN-BINDING, KELCH REPEAT, F-BOX PROTEIN 1
FLOWERING LOCUS C
FLOWERING LOCUS KH DOMAIN
FLOWERING LOCUS M
FLOWERING LOCUS T
HIGH EXPRESSION OF OSMOTICALLY RESPONSIVE GENES 1
LATE ELONGATED HYPOCOTYL
maltose binding protein
REPRESSOR OF GA1
SUPPRESSOR OF CONSTANS OVEREXPRESSION 1
SHORT VEGETATIVE PAHSE
TIMING OF CAB EXPRSSION 1
yellow fluorescence protein
Mouradov A, Cremer F, Coupland G. Control of flowering time: interacting pathways as a basis for diversity. Plant Cell. 2002;14:S111–30.
Amasino R. Seasonal and developmental timing of flowering. Plant J. 2010;61(6):1001–13.
Andrés F, Coupland G. The genetic basis of flowering responses to seasonal cues. Nat Rev Genet. 2012;13(9):627–39.
Moon J, Lee H, Kim M, Lee I. Analysis of flowering pathway integrators in Arabidopsis. Plant Cell Physiol. 2005;46(2):292–9.
Corbesier L, Coupland G. The quest for florigen: a review of recent progress. J Exp Bot. 2006;57(13):3395–403.
Song YH, Ito S, Imaizumi T. Flowering time regulation: photoperiod- and temperature-sensing in leaves. Trends Plant Sci. 2013;18(10):575–83.
Robson F, Costa MM, Hepworth SR, Vizir I, Piñeiro M, Reeves PH, et al. Functional importance of conserved domains in the flowering-time gene CONSTANS demonstrated by analysis of mutant alleles and transgenic plants. Plant J. 2001;28(6):619–31.
An H, Roussot C, Suárez-López P, Corbesier L, Vincent C, Piñeiro M, et al. CONSTANS acts in the phloem to regulate a systemic signal that induces photoperiodic flowering of Arabidopsis. Development. 2004;131(15):3615–26.
Yoo SK, Chung KS, Kim J, Lee JH, Hong SM, Yoo SJ, et al. CONSTANS activates SUPPRESSOR OF OVEREXPRESSION OF CONSTANS 1 through FLOWERING LOCUS T to promote flowering in Arabidopsis. Plant Physiol. 2005;139(2):770–8.
Putterill J, Robson F, Lee K, Simon R, Coupland G. The CONSTANS gene of Arabidopsis promotes flowering and encodes a protein showing similarities to zinc finger transcription factors. Cell. 1995;80(6):847–57.
Samach A, Onouchi H, Gold SE, Ditta GS, Schwarz-Sommer Z, Yanofsky MF, et al. Distinct roles of CONSTANS target genes in reproductive development of Arabidopsis. Science. 2000;288(5471):1613–6.
Valverde F, Mouradov A, Soppe W, Ravenscroft D, Samach A, Coupland G. Photoreceptor regulation of CONSTANS protein in photoperiodic flowering. Science. 2004;303(5660):1003–6.
Jang S, Marchal V, Panigrahi KC, Wenkel S, Soppe W, Deng XW, et al. Arabidopsis COP1 shapes the temporal pattern of CO accumulation conferring a photoperiodic flowering response. EMBO J. 2008;27(8):1277–88.
Liu LJ, Zhang YC, Li QH, Sang Y, Mao J, Lian HL, et al. COP1-mediated ubiquitination of CONSTANS is implicated in cryptochrome regulation of flowering in Arabidopsis. Plant Cell. 2008;20(2):292–306.
Lazaro A, Valverde F, Piñeiro M, Jarillo JA. The Arabidopsis E3 ubiquitin ligase HOS1 negatively regulates CONSTANS abundance in the photoperiodic control of flowering. Plant Cell. 2012;24(3):982–99.
Song YH, Smith RW, To BJ, Millar AJ, Imaizumi T. FKF1 conveys timing information for CONSTANS stabilization in photoperiodic flowering. Science. 2012;336(6084):1045–9.
Song YH, Shim JS, Kinmonth-Schultz HA, Imaizumi T. Photoperiodic flowering: time measurement mechanisms in leaves. Annu Rev Plant Biol. 2015;66:441–64.
Hicks KA, Millar AJ, Carré IA, Somers DE, Straume M, Meeks-Wagner DR, et al. Conditional circadian dysfunction of the Arabidopsis early-flowering 3 mutant. Science. 1996;274(5288):790–2.
Wang ZY, Tobin EM. Constitutive expression of the CIRCADIAN CLOCK ASSOCIATED 1 (CCA1) gene disrupts circadian rhythms and suppresses its own expression. Cell. 1998;93(7):1207–17.
Mizoguchi T, Wheatley K, Hanzawa Y, Wright L, Mizoguchi M, Song HR, et al. LHY and CCA1 are partially redundant genes required to maintain circadian rhythms in Arabidopsis. Dev Cell. 2002;2(5):629–41.
Strayer C, Oyama T, Schultz TF, Raman R, Somers DE, Más P, et al. Cloning of the Arabidopsis clock gene TOC1, an autoregulatory response regulator homolog. Science. 2000;289(5480):768–71.
Mizoguchi T, Wright L, Fujiwara S, Cremer F, Lee K, Onouchi H, et al. Distinct roles of GIGANTEA in promoting flowering and regulating circadian rhythms in Arabidopsis. Plant Cell. 2005;17(8):2255–70.
Suárez-López P, Wheatley K, Robson F, Onouchi H, Valverde F, Coupland G. CONSTANS mediates between the circadian clock and the control of flowering in Arabidopsis. Nature. 2001;410(6832):1116–20.
Nelson DC, Lasswell J, Rogg LE, Cohen MA, Bartel B. FKF1, a clock-controlled gene that regulates the transition to flowering in Arabidopsis. Cell. 2000;101(3):331–40.
Fowler S, Lee K, Onouchi H, Samach A, Richardson K, Morris B, et al. GIGANTEA: a circadian clock-controlled gene that regulates photoperiodic flowering in Arabidopsis and encodes a protein with several possible membrane-spanning domains. EMBO J. 1999;18(17):4679–88.
Imaizumi T, Schultz TF, Harmon FG, Ho LA, Kay SA. FKF1 F-box protein mediates cyclic degradation of a repressor of CONSTANS in Arabidopsis. Science. 2005;309(5732):293–7.
Fornara F, Panigrahi KC, Gissot L, Sauerbrunn N, Rühl M, Jarillo JA, et al. Arabidopsis DOF transcription factors act redundantly to reduce CONSTANS expression and are essential for a photoperiodic flowering response. Dev Cell. 2009;17(1):75–86.
Yanovsky MJ, Kay SA. Molecular basis of seasonal time measurement in Arabidopsis. Nature. 2002;419(6904):308–12.
Portolés S, Más P. Altered oscillator function affects clock resonance and is responsible for the reduced day-length sensitivity of CKB4 overexpressing plants. Plant J. 2007;51(6):966–77.
Sawa M, Kay SA. GIGANTEA directly activates Flowering Locus T in Arabidopsis thaliana. Proc Natl Acad Sci U S A. 2011;108(28):11698–703.
Johansson M, Staiger D. SRR1 is essential to repress flowering in non-inductive conditions in Arabidopsis thaliana. J Exp Bot. 2014;65(20):5811–22.
Kang MY, Yoo SC, Kwon HY, Lee BD, Cho JN, Noh YS, et al. Negative regulatory roles of DE-ETIOLATED1 in flowering time in Arabidopsis. Sci Rep. 2015;5:9728.
Park DH, Somers DE, Kim YS, Choy YH, Lim HK, Soh MS, et al. Control of circadian rhythms and photoperiodic flowering by the Arabidopsis GIGANTEA gene. Science. 1999;285(5433):1579–82.
Staiger D, Allenbach L, Salathia N, Fiechter V, Davis SJ, Millar AJ, et al. The Arabidopsis SRR1 gene mediates phyB signaling and is required for normal circadian clock function. Genes Dev. 2003;17(2):256–68.
Alabadí D, Oyama T, Yanovsky MJ, Harmon FG, Más P, Kay SA. Reciprocal regulation between TOC1 and LHY/CCA1 within the Arabidopsis circadian clock. Science. 2011;293(5531):880–3.
Gendron JM, Pruneda-Paz JL, Doherty CJ, Gross AM, Kang SE, Kay SA. Arabidopsis circadian clock protein, TOC1, is a DNA-binding transcription factor. Proc Natl Acad Sci U S A. 2012;109(8):3167–72.
Niwa Y, Ito S, Nakamichi N, Mizoguchi T, Niinuma K, Yamashino T, et al. Genetic linkages of the circadian clock-associated genes, TOC1, CCA1 and LHY, in the photoperiodic control of flowering time in Arabidopsis thaliana. Plant Cell Physiol. 2007;48(7):925–37.
Lu SX, Webb CJ, Knowles SM, Kim SH, Wang Z, Tobin EM. CCA1 and ELF3 interact in the control of hypocotyl length and flowering time in Arabidopsis. Plant Physiol. 2012;158(2):1079–88.
Michael TP, Salomé PA, Yu HJ, Spencer TR, Sharp EL, McPeek MA, et al. Enhanced fitness conferred by naturally occurring variation in the circadian clock. Science. 2003;302(5647):1049–53.
MacGregor DR, Gould P, Foreman J, Griffiths J, Bird S, Page R, et al. HIGH EXPRESSION OF OSMOTICALLY RESPONSIVE GENES1 is required for circadian periodicity through the promotion of nucleo-cytoplasmic mRNA export in Arabidopsis. Plant Cell. 2013;25(11):4391–404.
Carpenter CD, Kreps JA, Simon AE. Genes encoding glycine-rich Arabidopsis thaliana proteins with RNA-binding motifs are influenced by cold treatment and an endogenous circadian rhythm. Plant Physiol. 1994;104(3):1015–25.
Millar AJ, Kay SA. Circadian control of cab gene transcription and mRNA accumulation in Arabidopsis. Plant Cell. 1991;3(5):541–50.
Scortecci KC, Michaels SD, Amasino RM. Identification of a MADS-box gene, FLOWERING LOCUS M, that represses flowering. Plant J. 2001;26(2):229–36.
Fujiwara S, Oda A, Yoshida R, Niinuma K, Miyata K, Tomozoe Y, et al. Circadian clock proteins LHY and CCA1 regulate SVP protein accumulation to control flowering in Arabidopsis. Plant Cell. 2008;20(11):2960–71.
Michaels SD, Amasino RM. Loss of FLOWERING LOCUS C activity eliminates the late-flowering phenotype of FRIGIDA and autonomous pathway mutations but not responsiveness to vernalization. Plant Cell. 2001;13(4):935–41.
Pruneda-Paz JL, Breton G, Para A, Kay SA. A functional genomics approach reveals CHE as a component of the Arabidopsis circadian clock. Science. 2009;323(5920):1481–5.
Schaffer R, Ramsay N, Samach A, Corden S, Putterill J, Carré IA, et al. The late elongated hypocotyl mutation of Arabidopsis disrupts circadian rhythms and the photoperiodic control of flowering. Cell. 1998;93(7):1219–29.
Lu SX, Knowles SM, Andronis C, Ong MS, Tobin EM. CIRCADIAN CLOCK ASSOCIATED1 and LATE ELONGATED HYPOCOTYL function synergistically in the circadian clock of Arabidopsis. Plant Physiol. 2009;150(2):834–43.
Seaton DD, Smith RW, Song YH, MacGregor DR, Stewart K, Steel G, et al. Linked circadian outputs control elongation growth and flowering in response to photoperiod and temperature. Mol Syst Biol. 2015;11(1):776.
Knowles SM, Lu SX, Tobin EM. Testing time: can ethanol-induced pulses of proposed oscillator components phase shift rhythms in Arabidopsis? J Biol Rhythms. 2008;23(6):463–71.
Green RM, Tobin EM. Loss of the circadian clock-associated protein 1 in Arabidopsis results in altered clock-regulated gene expression. Proc Natl Acad Sci U S A. 1999;96(7):4176–9.
Wang W, Barnaby JY, Tada Y, Li H, Tör M, Caldelari D, et al. Timing of plant immune responses by a central circadian regulator. Nature. 2011;470(7332):110–4.
Burgess A, Searle I. The clock primes defense at dawn. Immunol Cell Biol. 2011;89(6):661–2.
Dai S, Wei X, Pei L, Thompson RL, Liu Y, Heard JE, et al. BROTHER OF LUX ARRHYTHMO is a component of the Arabidopsis circadian clock. Plant Cell. 2011;23(3):961–72.
Yakir E, Hilman D, Kron I, Hassidim M, Melamed-Book N, Green RM. Posttranslational regulation of CIRCADIAN CLOCK ASSOCIATED1 in the circadian oscillator of Arabidopsis. Plant Physiol. 2009;150(2):844–57.
Takada S, Goto K. TERMINAL FLOWER2, an Arabidopsis homolog of heterochromatin protein1, counteracts the activation of FLOWERING LOCUS T by CONSTANS in the vascular tissues of leaves to regulate flowering time. Plant Cell. 2003;15(12):2856–65.
Kwon YJ, Park MJ, Kim SG, Baldwin IT, Park CM. Alternative splicing and nonsense-mediated decay of circadian clock genes under environmental stress conditions in Arabidopsis. BMC Plant Biol. 2014;14:136.
Udvardi MK, Czechowski T, Scheible WR. Eleven golden rules of quantitative RT-PCR. Plant Cell. 2008;20(7):1736–7.
Jung JH, Lee S, Yun J, Lee M, Park CM. The miR172 target TOE3 represses AGAMOUS expression during Arabidopsis floral patterning. Plant Sci. 2014;215–216:29–38.
Yoo SD, Cho YH, Sheen J. Arabidopsis mesophyll protoplasts: a versatile cell system for transient gene expression analysis. Nat Protoc. 2007;2(7):1565–72.
Jefferson RA, Kavanagh TA, Bevan MW. GUS fusions: beta-glucuronidase as a sensitive and versatile gene fusion marker in higher plants. EMBO J. 1987;6(13):3901–7.
Park J, Kim YS, Kim SG, Jung JH, Woo JC, Park CM. Integration of auxin and salt signals by the NAC transcription factor NTM2 during seed germination in Arabidopsis. Plant Physiol. 2011;156(2):537–49.
Seo PJ, Park MJ, Lim MH, Kim SG, Lee M, Baldwin IT, et al. A self-regulatory circuit of CIRCADIAN CLOCK-ASSOCIATED1 underlies the circadian clock regulation of temperature responses in Arabidopsis. Plant Cell. 2012;24(6):2427–42.
This work was supported by the Leaping Research (NRF-2015R1A2A1A05001636) and Global Research Lab (NRF-2012K1A1A2055546) Programs provided by the National Research Foundation of Korea and the Next-Generation BioGreen 21 Program (PJ0111532015) provided by the Rural Development Administration of Korea. KEG was partially supported by Global PH.D Fellowship Program through the National Research Foundation of Korea (NRF-2015H1A2A1034250).
Availability of supporting data
The data sets supporting the results of this article are included within the article and its additional files.
CMP conceived and designed the project. MJP and YJK performed the molecular and biochemical assays. YJK and KEG measured flowering time of the mutants. CMP, MJP, YJK analyzed the data. CMP and MJP wrote the manuscript. All authors discussed the results and approved the final form of the manuscript.
The authors declare that they have no competing interests.
Consent to publish
Circadian rhythms in LHY-defective mutants. Ten-day-old plants grown on ½ X Murashige and Skoog-agar plates (hereafter, referred to as MS-agar plates) under long days (LDs, 16-h light and 8-h dark) were transferred to continuous light conditions at dawn (upper diagram). DAC, days after cold imbibition. Whole plants materials were harvested at the indicated zeitgeber time (ZT) points for total RNA extraction (lower panel). Rhythmic expression of CHLOROPHYLL A/B-BINDING PROTEIN 2 (CAB2) and CAROTENOID AND CHLOROPLAST REGULATION 2 (CCR2) genes, which exhibit circadian rhythmic expression patterns [41, 42], was examined by quantitative real-time RT-PCR (qRT-PCR). Biological triplicates were averaged. Bars indicate standard error of the mean. Two LHY-defective mutants (lhy-7 and lhy-20) were examined. (PDF 157 kb)
Expression of flowering time genes in lhy-7 mutant. Plants were grown under either LDs or short days (SDs, 8-h light and 16-h dark) for 10 days on MS-agar plates. Whole plants were harvested at ZT 8 for total RNA extraction. Transcript levels were examined by qRT-PCR. Biological triplicates were averaged and statistically treated using Student t-test (*P < 0.01). Bars indicate standard error of the mean. (PDF 131 kb)
Levels of LHY and CCA1 transcripts in 35S:LHY-MYC and 35S:MYC-CCA1 transgenic plants, respectively. Ten-day-old whole plants grown on MS-agar plates under LDs were harvested for total RNA extraction at the indicated ZT points. Transcript levels were examined by qRT-PCR. Biological triplicates were averaged and statistically treated (t-test, *P < 0.01). Bars indicate standard error of the mean. (PDF 121 kb)
Functionality of 35S:MYC-CCA1 and 35S:LHY-MYC transgenic plants. A and B. Elongated hypocotyls. Plants were grown on MS-agar plates for 5 days under either LDs (A) or SDs (B). Measurements of 20 seedlings were averaged and statistically treated (t-test, *P < 0.01). Bars indicate standard error of the mean. C. Disruption of circadian rhythms. Expression patterns of CCR2 gene were examined as described in Additional file 1. Bars indicate standard error of the mean. D. Suppression of FT transcription. Plants were grown under LDs for 10 days on MS-agar plates. Whole plants were harvested at ZT16 for total RNA extraction. Transcript levels were examined as described in Additional file 2. Bars indicate standard error of the mean. (PDF 195 kb)
Recombinant proteins used for electrophoretic mobility shift assay (EMSA). Recombinant maltose-binding protein (MBP) and MBP-CCA1 fusion protein were prepared in E. coli cells and affinity-purified. Protein quality was verified by running on 10 % SDS-PAGE and Coomassie brilliant blue staining. The arrow and arrowhead indicate full-size MBP and MBP-CCA1 proteins, respectively. SM, size marker. kDa, kilodalton. (PDF 263 kb)
EMSA on binding of MBP and MBP-CCA1 proteins to conserved sequences in FT locus. Recombinant MBP and MBP-CCA1 fusion proteins were prepared as described in Additional file 5. Radio-labelled CCA1-binding sequence (CBS) and evening element (EE) DNA fragments, which were described in Fig. 4a, were used. A. EMSA on MBP binding to DNA fragments. (+) and (−) indicate assays with or without MBP protein. Note that MBP alone does not bind to the CBS and EE sequences. B. EMSA on MBP-CCA1 binding to DNA fragments. The core sequences of CBS and EE were mutated, resulting in mCBS and mEE, respectively. Excess amounts (50X, 100X) of unlabeled DNA fragments were added as competitors. (PDF 182 kb)
ChIP assays on LHY binding to GI promoter. Chromatins were prepared from 7-day-old whole plants grown on MS-agar plates and immunoprecipitated using an anti-MYC antibody. Fragmented genomic DNA was eluted from the protein-DNA complexes and subjected to quantitative PCR. Biological triplicates were averaged and statistically treated using Student t-test (*P < 0.01). Bars indicate standard error of the mean. GI (NB) amplifies a downstream sequence region of GI gene, and GI (CBS) amplifies a sequence region containing CBS in the GI promoter, which has been described previously . (PDF 122 kb)
Expression of flowering genes in lhy-7 mutant under short days of 20-h total duration. Plants were grown for 10 days under short-day cycles of either 24-h (8-h light and 16-h dark) or 20-h (6.7-h light and 13.3-h dark) total duration. Whole plant materials were harvested throughout the % light-dark (L/D) cycles. Transcript levels were examined by qRT-PCR in Col-0 plants (A) and lhy-7 mutant (B). Biological triplicates were averaged. Bars indicate standard error of the mean. h, hour. (PDF 133 kb)
Expression of flowering genes in lhy-7 mutant under SDs of 20-h total duration. Plants were grown for 10 days under short-day cycles of 20-h total duration (6.7-h light and 13.3-h dark). Whole plant materials were harvested for total RNA extraction. Transcript levels were examined by qRT-PCR. Biological triplicates were averaged and statistically treated using Student t-test (*P < 0.01). Bars indicate standard error of the mean. (PDF 130 kb)
Primers used in qRT-PCR, RT-PCR, and ChIP-qPCR. F, forward primer; R, reverse primer. (PDF 90 kb)
About this article
Cite this article
Park, MJ., Kwon, YJ., Gil, KE. et al. LATE ELONGATED HYPOCOTYL regulates photoperiodic flowering via the circadian clock in Arabidopsis . BMC Plant Biol 16, 114 (2016). https://doi.org/10.1186/s12870-016-0810-8
- Arabidopsis thaliana
- Circadian clock
- Flowering time