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Brassinosteroids (BRs) regulate plant growth and stress responses via the BES1/BZR1 family of transcription factors, which regulate the expression of thousands of downstream genes. BRs are involved in the response to drought, however the mechanistic understanding of interactions between BR signalling and drought response remains to be established. Here we show that transcription factor RD26 mediates crosstalk between drought and BR signalling. When overexpressed, BES1 target gene RD26 can inhibit BR-regulated growth. Global gene expression studies suggest that RD26 can act antagonistically to BR to regulate the expression of a subset of BES1-regulated genes, thereby inhibiting BR function. We show that RD26 can interact with BES1 protein and antagonize BES1 transcriptional activity on BR-regulated genes and that BR signalling can also repress expression of RD26 and its homologues and inhibit drought responses. Our results thus reveal a mechanism coordinating plant growth and drought tolerance.
Brassinosteroids (BRs) are a group of plant steroid hormones regulating plant growth, development and responses to biotic and abiotic stresses1,2. Over the past two decades, the main components of the BR signalling pathway have been identified and characterized3,4,5,6,7,8,9,10,11,12,13,14,15,16,17,18,19,20,21,22. BR signalling leads to the accumulation of BES1/BZR1 (BRI1 EMS SUPPRESSOR 1/BRASSINAZOLE RESISTANT 1) family transcription factors in the nucleus to control the expression of target genes for BR responses23,24,25,26,27,28.
Several studies indicated that treatment of exogenous BRs could enhance the tolerance of plants to drought1,29,30. However, BR-deficient mutants were reported to have an enhanced tolerance to drought31,32,33, suggesting an inhibitory effect of BRs on drought tolerance. These early studies imply complex relationships between BR-regulated growth and drought responses. Several transcription factors, including drought-induced transcription factor RD26 (RESPONSIVE TO DESICCATION 26) and several of its close homologues, have been identified as the direct targets of BES1 and BZR1 (refs 23, 24), suggesting that these proteins may play important roles in interactions between BR and drought pathways.
RD26 belongs to the NAC (No apical meristem, Arabidopsis transcription activation factor and cup-shaped cotyledon) family of transcription factors, which are induced by drought, abscisic acid, NaCl and jasmonic acid34,35,36,37. Reporter gene expression studies showed that RD26 is expressed constitutively in both shoots and roots upon drought or salt stress treatments38,39. RD26 and its homologues function to promote drought-responsive gene expression and increase plant drought tolerance35. Recent studies showed that RD26 and its homologues, ANAC019 and ANAC055, are involved in plant bacterial pathogenesis, jasmonic acid-mediated defence and thermotolerance37,38,39,40,41,42.
In this study, we confirmed that RD26 is a target gene of BES1 and negatively regulates the BR signalling pathway. RD26 affects BR-regulated gene expression when overexpressed globally by binding and antagonizing BES1 transcriptional activities. Loss-of-function mutants in the BR signalling pathway had higher drought tolerance, while gain-of-function mutants in the BR pathway exhibited lower drought tolerance compared with wild type (WT). These results suggest that RD26 inhibits BR-regulated plant growth and the BR pathway also negatively regulates drought tolerance, establishing a mechanism for crosstalk between these two important pathways for plant growth and stress responses.
Previous ChIP–chip studies indicated that RD26 was a target of BES1 and BZR1, and its expression was repressed by BL (brassinolide, the most active BR), BES1 and BZR1 (refs 23, 24). Since BES1 and BZR1 can bind to BRRE to repress gene expression, we examined the RD26 gene promoter and found a BRRE site at nucleotide position −851 relative to the transcriptional start site. Chromatin immunoprecipitation (ChIP) experiments showed that BES1 binds to the BRRE site in vivo, with more binding in bes1-D in which BES1 protein accumulates than in WT plants (Supplementary Fig. 1a). RD26 expression was reduced by BL in WT plants and was repressed in bes1-D (Supplementary Fig. 1b). These results confirm that RD26 is a target of BES1, and its expression is repressed by BL through BES1.
Our previous result indicated that the loss-of-function rd26 mutant has a small increase in BR response23, suggesting that RD26 functions with its homologues to inhibit BR response. To confirm this hypothesis, we generated RD26 overexpression transgenic lines. RD26-overexpressing plants (RD26OX) displayed a stunted growth phenotype, the severities of which correspond well with RD26 protein levels (Fig. 1a). Moreover, the RD26OX transgenic plants could suppress the phenotype of bes1-D, a gain-of-function mutant in the BR pathway (Fig. 1b). Western blotting indicated that BES1 protein levels and phosphorylation status did not change significantly in bes1-D RD26OX double mutant (Fig. 1c). These results suggest that RD26 functions downstream of BES1 to inhibit BR-mediated growth.
To confirm that the RD26OX phenotype is related to reduced BR response, we determined its response to BL and to the BR biosynthesis inhibitor brassinazole (BRZ), which reduces endogenous BR levels43. RD26 overexpression plants have reduced response to BL in hypocotyl elongation assays (Fig. 1d). Likewise, RD26OX seedlings had shorter hypocotyls and were more sensitive to BRZ compared with Col-0 WT (Fig. 1e). Several RD26 homologues, ANAC019, ANAC055 and ANAC102, are also BES1 and/or BZR1 direct targets, and are repressed by BRs likely functioning redundantly in BR responses23,24. We generated quadruple mutant of rd26 anac019 anac055 anac102. The quadruple mutant has a BR-response phenotype and showed increased response to BL (especially at 100nM BL) compared with WT (Fig. 1d). The rd26 anac019 anac055 anac102 quadruple mutant is less sensitive to BRZ, especially at higher concentrations (Fig. 1e and Supplementary Fig.1c). The genetic evidence demonstrates that RD26 and its close homologues play a negative role in the BR signalling pathway.
To determine whether the strong phenotype of RD26OX plants is indeed related to BR response, we examined several known BR-induced genes by quantitative PCR (qPCR; Supplementary Fig. 2a). In general, many BR-induced genes we tested are downregulated in RD26OX, including genes involved in BR-regulated cell elongation (TCH4 and EXPL2), supporting a role of RD26 in modulating BR-regulated gene expression and plant growth. To more fully understand how RD26 negatively regulates BR responses, we performed global gene expression studies with RD26 mutants in the absence or presence of BRs by high-throughput RNA-sequencing (RNA-seq). We used 4-week-old adult plants for gene expression studies because RD26OX plants display the most obvious growth phenotype at this stage. In WT, 2,678 genes were induced and 2,376 genes were repressed by BL, among ~22,000 genes analysed (Fig. 2 and Supplementary Data 1 and 2), as we previously reported44. The BR-regulated genes from our RNA-seq analysis in adult plants have significant overlaps (~43%) with previous microarray analyses of BR-regulated genes in either seedlings or adult plants (Supplementary Data 3 and 4 and Supplementary Fig. 2b)24,45,46,47,48,49. Consistent with the strong phenotype of RD26OX plants, 3,246 genes are upregulated and 5,479 genes are downregulated in the transgenic plants, respectively (Fig. 2 and Supplementary Data 5 and 6).
To explore how RD26 affects BR-regulated gene expression, we examined the overlaps between BR-regulated genes and genes affected in RD26OX plants by performing clustering analysis with specific gene groups. RD26 modulates BR-responsive genes in complex ways (Fig. 2 and Supplementary Fig. 3). Consistent with the negative role of RD26 in BR response, 43% (1,141, Group 1) of BR-induced genes were downregulated in RD26OX plants and their induction by BRs was reduced, but not abolished (Fig. 2a,b). In contrast, only 20% (539, Group 3) of BR-induced genes were upregulated in RD26OX (Fig. 2a and Supplementary Fig. 3a). These results suggest that RD26 negatively modulates a significant portion of BR-induced genes.
On the other hand, among 2,376 BR-repressed genes, 595 (25%, Group 2) were upregulated and 823 (35%, Group 4) were downregulated in RD26OX plants (Fig. 2c,d and Supplementary Fig. 3b). While Group 3 and Group 4 genes suggest a positive role for RD26 in BR response (that is, BR-induced genes are upregulated and BR-repressed genes are downregulated in RD26OX), Group 1 and Group 2 genes demonstrated a negative role of RD26 in BR response (BR-induced genes are downregulated and BR-repressed genes are upregulated in RD26OX). In this study, we focus on the Group 1 and Group 2 genes to determine the mechanisms by which RD26 negatively regulates BR responses.
Consistent with the relatively weak BR-response phenotype of the rd26 anac019 anac055 anac102 mutant, only 405 genes are upregulated and 378 are downregulated in rd26 anac019 anac055 anac102 quadruple mutant (Supplementary Fig. 4 and Supplementary Data 7 and 8). We further compared BR-regulated genes and genes affected in RD26OX and the rd26 anac019 anac055 anac102 mutant (Supplementary Fig. 5a,b). Four subgroups are subjected to further clustering analysis: BR-induced genes that are downregulated in RD26OX and upregulated in the quadruple mutant (36, Supplementary Fig. 5c); BR-induced genes that are upregulated in RD26OX and downregulated in the quadruple mutant (15, Supplementary Fig. 5e); BR-repressed genes that are upregulated in RD26OX and downregulated in the quadruple mutant (44, Supplementary Fig. 5d); and BR-repressed genes that are downregulated in RD26OX and upregulated in the quadruple mutant (19, Supplementary Fig. 5f). Most of these genes are affected in opposite ways in the rd26 anac019 anac055 anac102 mutant and RD26OX. These results support the conclusion that RD26 and its homologues function in a complex way to modulate BR-regulated gene expression.
Previous studies indicated that both BES1 and BZR1 can bind to the BRRE site or E-boxes to inhibit or activate gene expression, respectively23,24. We examined the Group 1 and Group 2 gene promoters and found that BRRE elements are especially enriched in Group 2 gene promoters (Supplementary Fig. 6a and Supplementary Table 1) and E-boxes (CANNTG, especially a specific E-box CATGTG in BR-induced gene promoters28) are enriched in Group 1 gene promoters (Supplementary Fig. 6b,c and Supplementary Table 1), within 500 base pairs (bp) relative to the transcriptional start sites. The differential enrichments within −500bp promoter regions are significant as most BES1- and BZR1-binding sites are located in the region as revealed by genome-wide ChIP–chip studies23,24. We selected several gene promoters from Group 1 and Group 2 and fused with luciferase (LUC) gene to generate reporter constructs. BES1, RD26 or BES1 plus RD26 were co-expressed with the reporter constructs and the reporter gene expression was determined. While BES1 repressed and RD26 activated the expression of Group 2 genes, the reporter gene expression level was in between when BES1 and RD26 were co-expressed (Fig. 3a–c). In contrast, BES1 activated and RD26 repressed Group 1 reporter genes, and the expression level fell in the middle when RD26 and BES1 were co-expressed (Fig. 3d–f). These results indicated that RD26 acts to antagonize BES1 actions on these BR-regulated genes.
To reveal the mechanisms by which RD26 inhibits the large number of BR-induced genes (Group 1, Fig. 2b) and upregulates many BR-repressed genes (Group 2, Fig. 2d), we chose one gene representative of each group for further mechanistic studies. A BR-repressed gene, At4g18010, was chosen to represent Group 2 genes because it is upregulated in RD26OX and its promoter contains a BRRE site at −405bp relative to the transcription start site (Supplementary Fig. 7a). Likewise, A BR-induced gene At4g00360 was chosen to represent Group 1 genes as its promoter contains a well-established BES1-binding site, CATGTG E-box, at nucleotide −470 (Supplementary Fig. 7b).
To confirm the antagonistic effect of RD26 on BES1-mediated gene expression observed by LUC reporter gene assays, we examined the expression of these two genes in bes1-D, RD26OX and bes1-D RD26OX plants, in which BES1, RD26 or both are increased. As shown in Fig. 3g, the expression of At4g18010 was downregulated in bes1-D and upregulated in RD26OX, but the expression level was in between in bes1-D RD26OX double mutant. In contrast, the expression of At4g00360 was much higher in bes1-D compared with bes1-D RD26OX, while its expression was significantly repressed in RD26OX (Fig. 3h).
Previous DNA-binding experiments showed that NAC transcription factors including RD26 (ANAC072) and ANC019 could bind to DNA sequences with two motifs—CATGT(G) and a CACG core spaced by varying numbers of nucleotides35,41,42. The NAC-binding sites are very similar to E-box (CANNTG) or conserved core sequence of the BRRE site (CGTGT/CG), well-established binding sites for BES1/BZR1 (refs 23, 24). These results suggest that RD26 and BES1 could potentially bind to the same site to modulate BR-regulated gene expression.
We first used yeast one-hybrid assays to test whether BES1 and RD26 can target to the same promoter fragments (Fig. 4). We fused several fragments of the At4g18010 promoter (-P1, -P2 and -P3, with BRRE located in P3) and At4g00360 promoter (-P1, -P2 and -P3, with CACGTG E-box located in P3) to pLacZi reporter (Clontech Inc.) and integrated them into the yeast genome (Fig. 4a). Mutants were also generated in which At4g18010-P3 BRRE and At4g00360-P3 E-box were mutated to unrelated sequences (see Fig. 5a). BES1 (with pGBKT7 vector), RD26 (with pGADT7 vector) or both BES1 and RD26 were expressed in each of the reporter yeast strain and the LacZ expression was determined. As shown in Fig. 4b, while neither BES1 nor RD26 significantly changed the gene expression from At4g18010-P3, co-expression of BES1 and RD26 activated the reporter gene expression. It is worth noting that the fusion of the GAL4 activation domain in pGADT7 to RD26 apparently changed RD26 property in yeast to become an activator in combination with BES1 (compared with the result from plants in Fig. 3), which is necessary to detect BES1/RD26 interaction in yeast. Moreover, mutation of the BRRE in At4g18010-P3 completely abolished the activation (Fig. 4b). The results demonstrated that BES1 and RD26 act through the BRRE site in the At4g18010-P3 promoter fragment. Similarly, co-expression of BES1 and RD26 activated At4g00360-P3 reporter, which is much reduced when the CATGTG E-box is mutated, indicating that BES1 and RD26 act through the CATGTG E-box in At4g00360-P3 (Fig. 4c) to regulate gene expression.
We also performed ChIP assays with WT and RD26OX transgenic plants, with BES1 antibody23 or RD26 antibodies we generated (Supplementary Fig. 8). While BES1 itself binds to the At4g18010 promoter (P3) in WT plants, such binding is enhanced in RD26OX plants (Fig. 4d, columns 3 and 4), suggesting that BES1 and RD26 together enhance binding to the promoter region. Consistent with the result that RD26 antibody detects RD26 in RD26OX but not in WT plants (Supplementary Fig. 8a,b), RD26 binding to the At4g18010 promoter (P3) in RD26OX was strongly apparent but barely detectable in WT (Fig. 4d, columns 5 and 6). In contrast, such cooperative binding is not detected in the more upstream promoter region (Fig. 4d, columns 9–12).
To confirm that BES1 and RD26 can bind to the same promoter regions at the same time, we also performed ChIP–reChIP with chromatin prepared from RD26OX, rd26 anac019 anac055 anac102 (rdQ) or BES1 RNAi plants in which the BES1 level is reduced27 (Supplementary Fig. 9). When the first ChIP was performed with anti-BES1 antibody and eluted chromatin samples were then immunoprecipitated with anti-RD26 or IgG control, significant enrichment of BES1/RD26 binding was detected in RD26OX plants, which is clearly reduced in rdQ mutant, and moderately reduced in BES1RNAi plants with two pairs of independent qPCR primers (Supplementary Fig. 9a,b). Similar results were obtained when the first ChIP was performed with anti-RD26 antibody and reChIP with anti-BES1 (Supplementary Fig. 9c). These results suggest that BES1 and RD26 can simultaneously bind to the At4g18010 gene promoter in vivo.
To further reveal the biochemical mechanisms by which RD26 antagonizes BES1 actions, electrophoretic mobility shift assay (EMSA) experiments were performed with recombinant BES1 and RD26 proteins using DNA probes containing BRRE (from At4g18010) or CATGTG E-box (from At4g00360; Fig. 5a and Supplementary Fig. 10). While BES1 binds to BRRE (CGTGTG) from At4g18010 quite strongly, RD26 binds to the probe more weakly; moreover, both bindings were abolished with mutant probe in which BRRE is mutated (Fig. 5b). Interestingly, BES1 and RD26 together can bind to the BRRE probe more strongly, and the binding is also abolished when the BRRE site is mutated (Fig. 5b). Similar results were obtained with probe containing CATGTG E-box from At4g00360. While RD26 and BES1 can each bind to E-box site separately, RD26 and BES1 synergistically bind to WT but not mutated E-box probe (Fig. 5c). Since BES1 (335 aa) and RD26 (298 aa) are similar in predicted protein sizes, the strong bands when both proteins are present more likely represent heterodimer of the two proteins, while each of them likely bind to the probe as homodimer. Taken together, the DNA binding and gene expression results suggest that RD26 interacts with BES1 on BRRE site to inhibit BES1's repression function (Fig. 5d) and on E-box to inhibit BES1's activation function (Fig. 5e).
The yeast one-hybrid and DNA-binding experiments described above suggest that BES1 and RD26 may be able to interact with each other. To test this hypothesis, we expressed full-length or truncated BES1 with MBP, and RD26 and truncations with Glutathione S-transferase tag, respectively (Fig. 6a). Glutathione S-transferase pull-down assays indicated that full-length RD26 could interact with full-length BES1 protein (Fig. 6b). The domains involved in DNA binding/dimerization of BES1 (aa 1–89) and RD26 (aa 1–140) are sufficient for the interaction (Fig. 6c). Split Luciferase (Luc) assay was used to test whether RD26 and BES1 interact in plants50. RD26 was fused with the amino part of Luc (NLuc) and BES1 was fused with carboxyl-part of Luc (CLuc), respectively (Fig. 6d). Co-expression of RD26-NLuc and CLuc-BES1 in tobacco leaves led to increased Luc activity, while co-expression of controls (RD26-NLuc with CLuc or CLuc-BES1 with NLuc) only produced background-level activities (Fig. 6e).
We further confirmed that BES1 and RD26 interaction in vivo by co-immunoprecipitation and by BiFC experiments. GFP antibody (tagged to BES1) can specifically pull down RD26-MYC co-expressed in tobacco leaves (Fig. 6f). In BiFC assays, co-expression of BES1-YFPN and RD26-YFPC lead to reconstitution of yellow fluorescence protein (YFP) signal in the nucleus (Fig. 6g,h), but YFP signals were not observed in BES1-YFPN/YFPC or YFPN/RD26-YFPC controls (Fig. 6i–l). Taken together, these results indicated that BES1 and RD26 can interact with each other through corresponding DNA-binding/dimerization domains and inhibit each other's functions on Group 1 and Group 2 genes.
Since BRs function through BES1/BZR1 to repress the expression of RD26 and its homologues, we tested whether the BR pathway affects plant drought response. Previous data showed that the expression of RD26 was induced by drought29,30,35,38. Drought induces 2,503 and represses 2,862 genes (combination of 2- and 3-day drought treatment data, Supplementary Data 9 and 10)51. Analysis of gene expression affected in RD26OX and drought-regulated genes revealed that RD26 upregulated 38% (963) of drought-induced genes, but only 12% (346) of drought-repressed genes; similarly, RD26 downregulated 45% (1299) of drought-repressed genes, but only 19% (488) of drought-induced genes (Supplementary Fig. 11). The results suggest that RD26 plays a major role in plant drought responses.
We also compared BR-regulated genes and drought-regulated genes and found that ~38% of BR-regulated genes are modulated by drought (Supplementary Fig. 12). If BR signalling indeed inhibits drought response, we expect that loss-of-function BR mutants have increased, and gain-of-function mutants have decreased, drought tolerance. BR loss-of-function mutant, bri1-5, a weak BR receptor mutant52, was exposed to drought stress. After drought stress and recovery, 50% of bri1-5 mutant plants survived, compared with 16% for WT (Fig. 7a, top panel). On the other hand, a gain-of-function mutant in the BR pathway, bes1-D, showed less drought tolerance. Only 22% of bes1-D mutants survived, but all of WT controls survived in the drought stress experiment (Fig. 7a, bottom panel). The drought response phenotypes were also confirmed in bes1-D in Col-0 background53 with the same trend (Supplementary Fig. 13).
To test our hypothesis that the BR signalling pathway inhibits drought response by repressing RD26 and its homologues, the expression of several drought-induced or drought-related genes were examined in bri1-5 mutant and bes1-D mutant. Transgenic plants overexpressing RD26/ANAC072, ANAC019 or ANAC055 could enhance the tolerance to drought stress, suggesting that RD26 and its homologues ANAC019 and ANAC055 are involved in drought response19. Reverse transcriptase qPCR (RT–qPCR) results showed that the expression of all three genes plus ANAC102 are increased in bri1-5 mutant and decreased in bes1-D mutant (Fig. 7b). We also examined five other genes involved in drought tolerance54. All five genes are upregulated in bri1-5 and downregulated in bes1-D (Fig. 7b). The results demonstrated that drought response genes are constitutively expressed in loss-of-function BR mutants and repressed in gain-of-function BR mutants, confirming that the BR signalling pathway inhibits drought response, likely by repressing the expression of RD26 and its homologues.
We examined the double-mutant bes1-D RD26OX and found that RD26 overexpression can clearly rescue the bes1-D phenotype in drought response (Supplementary Fig. 14a). Consistent with the facts that RD26OX suppress bes1-D phenotypes, several bes1-D-induced genes are downregulated in RD26OX plants (Supplementary Fig. 14b). The expression of these genes is also reduced in bes1-D RD26OX double-mutant compared with bes1-D (Supplementary Fig. 14b). The gene expression studies support the idea that RD26 suppresses bes1-D phenotypes.
To further understand the relationships among BES1 and RD26/its close homologues, we constructed a Gene Regulatory Network (GRN) based on gene expression correlations using BES1, RD26, ANAC019, ANAC055 and ANAC102 as seed genes55. The GRN showed that RD26 and three of its close homologues have extensive expression correlations, directly or through other genes (Fig. 7c). Interestingly, BES1 has relatively fewer connections to other genes; in addition, the ‘RD26/homologue cluster' and ‘BES1 cluster' are connected through only one gene, BOS1, which was implicated in plant responses to drought, high salinity and fungal pathogens54,56.
To validate the GRN, we compared the genes in the network with genes affected in RD26OX, as well as drought- and BR-regulated genes (Supplementary Fig. 15). Interestingly, 82% of the 103 genes in the GRN are affected in RD26OX, although only about one-third of total detected genes are affected in RD26 OX plants. Similarly, 72 and 52% of the genes in the GRN are either regulated by drought or BRs, despite the fact that only about one-fourth of total genes are regulated by drought or BRs. The computationally generated GRN and its validation by RNA-seq data support the conclusions that (1): there are close interactions between the BES1-mediated BR pathway and the drought pathway represented by RD26 and its homologues; (2) although the interactions between BES1 and RD26 can happen at a transcriptional level (that is, through BOS1), post-transcriptional regulations such as protein–protein interaction between RD26 and BES1 likely play a major role.
In this study, we found that the drought-responsive transcription factor RD26 is a target of BES1 and functions to inhibit BR responses. Gene expression studies revealed that RD26 and BES1 act antagonistically in the regulation of many BR-regulated genes. The antagonistic interactions happen at multiple levels. While BES1/BZR1 functions to repress the expression of RD26 at a transcription level, the RD26 protein interacts with BES1 and inhibits its transcriptional activity. Our results thus establish a molecular link and mechanism of interaction between BR and drought response pathways (Fig. 8).
Our genetic, genomic, molecular and biochemical results demonstrated that RD26 functions to inhibit the BR pathway (Fig. 8). RD26 is induced by drought, promotes drought-regulated gene expression and confers drought tolerance when overexpressed35,36. Our genetic studies demonstrate that RD26 is a negative regulator of the BR pathway as overexpression of RD26 leads to reduced plant growth and BR response and knockout of RD26 and three of its homologues lead to increased BR response. The relatively weak growth phenotype of rd26 anac019 anac055 anac102 mutant may be explained by additional family members, which possibly function redundantly in the inhibition of BR response. The fact that a smaller number of genes affected in rd26 anac019 anac055 anac102 mutant compared with RD26OX transgenic plants is consistent this hypothesis. RD26 and its homologues appear to function as part of a highly redundant and complex network to confer drought tolerance and to inhibit plant growth during drought stress.
Global gene expression studies revealed that RD26 functions to modulate BR-responsive gene expression in a complex manner, that is, RD26 can either activate or repress both BR-induced and BR-repressed genes. However, a large number of BR-induced genes (1,141 or 43% of BR-induced genes identified in this study) are significantly downregulated in RD26 OX (Group 1, Fig. 2). Our molecular and biochemical studies suggest that RD26 affects Group 1 gene expression by binding to the BES1 target site (E-box) and neutralizing BES1 activation activity, potentially by forming an inactive heterodimer (Figs 3, ,4,4, ,5).5). Likewise, 595 (or 25%) BR-repressed genes are upregulated in RD26OX, suggesting that BR and RD26 have opposite function on these genes (Group 2, Fig. 2). Indeed, the molecular and biochemical evidence suggests that, while BES1 binds to BRRE to repress gene expression, RD26 can antagonize BES1-mediated gene repression (Fig. 3). We also provided evidence that BES1 and RD26 protein can interact with each other in vitro and in vivo (Fig. 6). While many protein–protein interactions between transcription factors synergistically activate or repress transcription, our results suggest that BES1 and RD26 interact and antagonize each other's transcriptional activities on Group 1 and Group 2 gene promoters. Our findings thus reveal a previously unknown mechanism that two signalling pathways converge on the same promoter element through two interacting transcription factors to coordinate plant growth and stress responses. Consistent with our conclusion, recent ChIP-seq studies showed that RD26 target gene promoters under abscisic acid treatment are enriched in G-box sequence (CACGTG, a specialized E-box)57, very similar to BES1 target sites derived from ChIP–chip study23.
We also observed an inhibitory effect of the BR pathway on drought response as a loss-of-function BR mutant is resistant to drought and a gain-of-function mutant of the BR pathway had compromised drought response. The transcriptional repression of RD26 and its homologue genes by BRs likely play a major role in the observed inhibition of drought response by the BR pathway as the expression of RD26 and its homologues (including ANAC019, ANAC 055 and ANAC102) are significantly increased in bri1 and decreased in bes1-D (Fig. 7b). While we have provided experimental evidence that RD26 antagonizes BES1-mediated gene expression on the BES1 target sites, it remains to be determined whether BES1 inhibits RD26-mediated gene expression on RD26-related drought target genes.
We propose that the antagonistic interaction between BES1 and RD26 likely ensures that plant growth is reduced when plants are under drought stress, under which RD26 and its homologues are upregulated to inhibit BR-induced growth, thus allowing more resources to deal with the drought stress. On the other hand, under normal growth conditions, i.e., in the absence of drought stress, BR signalling represses the drought pathway by repressing the expression of RD26 and its homologues.
It is worth noting that RD26 and BES1 do not seem to act antagonistically at all times. For example, 539 BR-induced genes (20%, Group 3) are upregulated and 823 BR-repressed genes (35%, Group 4) are downregulated in RD26OX (Supplementary Fig. 3), indicating that RD26 and BES1 act in a similar manner on these two groups of genes. It is possible that RD26 and BES1 target different promoter elements to achieve the positive interactions between RD26 and BES1. It has been suggested that at least under some conditions exogenously applied BR can improve plant drought tolerance58. It is possible that under these circumstances the Group 2 and Group 4 genes play more dominant roles than Group 1 and Group 2 genes, which can potentially allow BR to activate some drought-induced genes and repress BR-repressed genes and thus promote drought tolerance. More investigation is needed to better understand the interaction between RD26 and BES1 on Group 3 and Group 4 genes.
In summary, we have identified RD26 as a molecular link that coordinates BR and drought responses. We further found that, while BES1 functions to repress RD26 gene expression, RD26 interacts with BES1 and inhibits BES1 transcriptional activity. This reciprocal inhibitory mechanism not only ensures that BR-induced growth is inhibited under drought conditions, but also prevents unnecessary activation of drought response when plants undergo BR-induced growth.
T-DNA insertion mutants, rd26 (At4g27410, SALK_063576), anac019 (At1g52890, SALK_096295), anac055 (At3g15500, SALK_014331) and anac102 (At5g63790, SALK_030702) were obtained from ABRC (Arabidopsis Biological Resource Center). All plants were grown on 1/2MS plates and/or in soil under long day conditions (16h light/8h dark) at 22°C. BRZ and BL response experiments were carried out as previous described59. Briefly, seeds were sterilized with 70% ethanol and 0.1% Triton X-100 for 15min and washed with 100% ethanol three times and dried in filter papers in a sterile hood. The seeds were sprinkled onto half Linsmaier and Skoog medium (Caisson Lab) with 0.7% Phytoblend agar (Caisson Lab) and various concentrations of BRZ (provided by Professor Tadao Asami) or BL (Wako Biochemical). Both BRZ and BL (1mM stock in dimethylsulphoxide) were added to medium after autoclave and the plates with seeds were placed at 4°C for 3 days. After exposing to light for 8h, the plates were wrapped with three layers of aluminium foil and incubated in the dark at 25°C for 5 days for BRZ response and in the constant light for 7 days for BL response experiments. Hypocotyls were scanned and measured using Image J (https://imagej.nih.gov/ij/). Ten to fifteen hypocotyls were measured, and averages and s.d. were calculated and plotted.
For MYC-tagged transgenic plants, RD26 genomic sequence including its 5′ UTR was cloned from WT and fused with MYC tag and CaMV 35S promoter into pZP211 vector60. For recombinant protein purification, full-length or fragments of RD26 and BES148-coding regions were cloned into the pETMALc-H vector61 or pET-42a (Novagen). All primers used in this study are provided in Supplementary Table 2.
The construct of RD26-MYC driven by 35S promoter was transformed into Agrobacterium tumefaciens (stain GV3101), which were used to transform plants by the floral dip method62. Transgenic lines were selected on 1/2 MS medium plus 60gml−1 gentamycin. Transgene expression was analysed by western blotting with 2μg anti-c-MYC (Sigma, C3956) antibody or HERK1 antibody as control. All the uncropped images for western blots in this study are provided in Supplementary Fig. 16. HERK1 kinase domain49 and full-length RD26 recombinant proteins were expressed from pETMALc-H and used to generate polyclonal antibody at the Iowa State University Hybridoma Facility (http://www.biotech.iastate.edu/biotechnology-service-facilities/hybridoma-facility/). About 2μg of affinity-purified antibody was used in each western blotting in 10ml.
For RD26, At4g00360 and At4g18010 gene expression, total RNA was extracted and purified from 2-week-old plants of different genotypes using the RNeasy Mini Kit (Qiagen). The Mx4000 multiplex Quantitative PCR System (Stratagene) and SYBR GREEN PCR Master Mix (Applied Biosystems) were used in quantitative real-time PCR analysis. For transient expression, promoters for At4g00360 (1,552bp) and At4g18010 (1,515bp), At1g22400 (1,922bp), At5g17860 (1,119bp), At4g14365 (430bp) and At3g19720 (411bp) were cloned and used to drive luciferase reporter gene expression. The BES1-coding region driven by CaMV 35S promoter was cloned into pZP211 vector, while RD26-MYC construct used in transgenic plant generation was also used in transient experiment. Tobacco leaf transient assay63 was used to examine the effect of RD26 and BES1 on reporter gene expression either with individual protein or with combination of BES1 and RD26. Equal amount of Agrobacterium cells (measured by OD600, adjusted to the same with vector-containing strain) were injected into the leaves of tobacco. The activities of the luciferase were measured in total protein extracts from triplicate samples (collected with a 5mm leaf puncher with same number of leaf discs in each sample) using Berthold Centro LB960 luminometer with the luciferase assay system following the manufacturer's instruction (Promega). The relative level of luciferase activity was normalized by the total amount protein for each sample.
For global gene expression, total RNA was extracted and purified from 4-week-old plants of different genotypes using the RNeasy Mini Kit (Qiagen). Duplicate RNA samples were subjected to RNA-seq using HiSeq2000 50bp single-end sequencing in the DNA facility at Iowa State University. Raw RNA-seq reads were subjected to quality-checking and trimming and then aligned to the Arabidopsis reference genome (TAIR10) using an intron-aware aligner, Genomic Short-read Nucleotide Alignment Program64. The alignment coordinates of uniquely aligned reads for each sample were used to independently calculate the read depth of each annotated gene. Genes with an average of at least one uniquely mapped read across samples were tested for differential expression using QuasiSeq (http://cran.r-project.org/web/packages/QuasiSeq). The generalized linear model Quasi-likelihood spline method assuming negative binomial distribution of read counts implemented in the QuasiSeq package was used to compute a P value for each gene. The 0.75 quantile of reads from each sample was used as the normalization factor65. A multiple test-controlling approach was used to convert P values to q-values for controlling false-discovery rate66. For most of the comparisons, q-values no larger than 0.05 were considered to be differentially expressed. Owing to the strong growth phenotype of RD26OX transgenic lines, more stringent (q<0.003) condition was used to determine differentially expressed genes. Clustering was performed using the ‘aheatmap' function of the NMF package in R (https://cran.r-project.org/web/packages/NMF/index.html). Log2 reads per million mapped read values were used for clustering analysis and values were normalized for each gene by centring and scaling each row of the heatmap. The overlapped genes were identified and displayed using Venny2.0 programme (http://bioinfogp.cnb.csic.es/tools/venny/).
ChIP was performed as previously described23 with modifications67. Briefly, 5g of 4-week-old plants were fixed in 1% formaldehyde and used to isolate nuclei and chromatin. The chromatin was sheared with Diagenode Bioruptor Sonication System with 30 cycles of 30-s on and 30-s off in icy water bath. Twenty micrograms of affinity-purified BES1 (ref. 23), RD26 antibodies (see ‘Generation and analysis of transgenic plants' section) or IgG (Sigma, I5006) were used to immunoprecipitate chromatin, which was collected with 20μl Dynabeads protein A (Invitrogen). Three qPCR technical repeats were used to calculate enrichment folds compared to ubiquitin control (UBQ5). The enrichment of specific transcription factors was examined by qPCR with primers from indicated regions. The averages and s.e.'s were derived from four biological repeats.
For ChIP–reChIP, chromatin was prepared from 15g RD26OX, BES1RNAi or rdQ mutant plants with a modified protocol in which the crosslinking with formaldehyde was performed after tissue grinding in liquid nitrogen, and all the buffer volumes were scaled up by 15-folds compared with the published protocol68. The sonication and immunoprecipitation were performed as described above with BES1 or RD26 antibody. Each first immunoprecipitated chromatin sample was eluted with 75μl 10mM Tris-HCl (pH 8.0), 1mM EDTA, 2% SDS and 15mM dithiothreitol and diluted 20-folds for second immunoprecipitation with corresponding antibody (RD26 or BES1) or IgG control. The enrichment at specific regions was determined by qPCR with indicated primers as described above. The averages and s.e.'s were derived from three biological repeats.
For promoter motif analysis, we downloaded Group 1 and 2 genes upstream 3kb sequence from TAIR database (https://www.Arabidopsis.org/tools/bulk/sequences/index.jsp). On the basis of this sequence information, we coded in-house Perl scripts to match possible E-box and BRRE motif in upstream 3,000bp region by searching conserved sequence ‘CANNTG' for general E-box or CATGTG for specific E-box and conserved sequence ‘CGTG(T/C)G' for the BRRE site. All the statistical analyses was done by R language (http://www.R-project.org/). We fitted a negative binominal model for fitting the frequency of E-box and BRRE domain in ‘glm.nb' function and then calculated P value for each comparison. The density plots were generated by R language ‘plot' function.
For re-analysis of previously published microarray data24,45,46,47,48,49, we downloaded the microarray raw CEL data from Riken and analysed the arrays using the ‘Robust Multi-array Average method'69 to obtain gene expression data. To analyse gene expression and compare the expression between the WT and hormone treatments, we used the linear model for microarray (limma) package from the Bioconductor project (http://www.bioconductor.org). When estimating statistical significance for log2-transformed fold-change replicates were combined analogous to the classical pooled two-sample t-test. To account for multiple testing, we used the Benjamini–Hochberg method, and significance level for detection is at 5%. The differential expressed genes were combined with published gene lists to obtain the BR-regulated genes by microarrays were and listed in Supplementary Data 3 and 4.
The Split Luciferase Complementation Assays were performed as described50. The coding region of RD26 and BES1 were cloned into the pCAMBIA1300-nLUC and pCAMBIA1300-cLUC constructs, respectively. Tobacco leaf transient assay was used to examine luciferase activity in the presence or absence of RD26 and/or BES1. Equal amount of Agrobacterium cells (measured by OD600, adjusted to same with vector-containing strain) were injected to tobacco leaves. The luciferase activities were measured from protein extracts from triplicate samples as described above. For the immunoprecipitation (IP) experiments, tobacco leaves were homogenized in protein lysis buffer (1mM EDTA, 10% glycerol, 75mM NaCl, 0.05% SDS, 100mM Tris-HCl, pH 7.4, 0.1% Triton X-100 and 1 × complete cocktail protease inhibitors). After protein extraction, anti-GFP antibody (10μl, Life Technologies-Molecular Probes, A21311) was added to total proteins. After incubation with gentle mixing for 1h at 4°C, 200μl fresh 50% slurry of protein A beads (Trisacryl Immobilized Protein A-20338, Thermo Scientific) were added, and incubation was continued for 1h. Protein A beads were pelleted by centrifugation at 2,000r.p.m. for 1min, and the supernatant was removed. The precipitated beads were washed at least four times with the protein extraction buffer and then eluted by 2 × SDS protein-loading buffer with boiling for 5min. The IP products were used for western blotting with 2μg of anti-BES1 antibody or MYC antibody (Sigma, C3956). BiFC experiments were performed as recently described44. BES1 and RD26 cDNAs were cloned into the N- or C terminus of EYFP vectors70. Sequencing-confirmed constructs were transformed into Agrobacterium tumefaciens strain GV3101. Agrobacteria were grown in LB medium containing 0.2M acetosyringone and washed with infiltration medium (10mM MgCl2, 10mM MES, pH 5.7, 0.2M acetosyringone) and resuspended to OD600 0.5 with infiltration medium. Combinations of Agrobacterium were infiltrated into Nicotiana benthamiana leaves and examined for YFP signals 2 days after infiltration. A Leica SP5 X MP confocal microscope equipped with an HCS PL APO CS 20.0 × 0.70 oil objective was used to detect reconstituted YFP. YFP was excited with a 514-nm laser line and detected from 530 to 560nm. The LAS AF software (Leica Microsystems) was used to obtain images with same settings.
EMSA experiments were carried out as described previously25. After annealing, oligonucleotide probes were labelled with P32-γ-ATP using T4 polynucleotide kinase. About 0.2ng probe and indicated amount of proteins purified from Escherichia coli were mixed in 20μl binding buffer (25mM HEPES-KOH (pH 8.0), 1mM DTT, 50mM KCl and 10% glycerol). After 40min incubation on ice, the reactions were resolved by 5% native polyacrylamide gels with 1 × TGE buffer (6.6gl−1 Tris, 28.6gl−1 glycine and 0.78gl−1 EDTA (pH 8.7)).
Drought stress tolerance experiments were carried out as described previously35 with minor modifications: different genotype plants were grown on 1/2 MS medium for 2 weeks, and then transferred to soil and grown for one more week in growth chamber (22°C, 60% relative humidity, long day conditions) before exposure to drought stress. Drought stress was imposed by withholding water until the lethal effect of dehydration was observed on WT control or bes1-D plants. The numbers of plants that survived and continued to grow were counted after watering for 7 days.
We first constructed a whole-genome network of Arabidopsis using the TINGe software55. To construct the Arabidopsis network, microarray data were collected from a total of 3,546 non-redundant Affymetrix ATH1 expression profiles. The data were subjected to statistical normalization and filtering, following which 15,495 genes remained for network construction. The RD26–BES1 subnetwork was then extracted from the whole-genome network using a subnetwork analysis tool, GeNA55. GeNA ranks each gene in the whole-genome network with respect to its relevance to a given set of seed genes and extracts a subnetwork containing the seed genes and genes of highest ranks with respect to the seed genes.
Matchmaker One-Hybrid System (Clontech) was used to test the binding of BES1/RD26 to At4g18010 and At4g00360 gene promoters following the manufacturer's instructions (http://download.bioon.com.cn/upload/month_0907/20090707_dab6285a579af1fb2ccd87zow1gx859t.attach.pdf). Briefly, promoter fragments were cloned into pLacZi (KpnI and SalI sites) and integrated into the genome of yeast strain YM4271 to generate reporter lines. Mutant reporter lines were also generated with promoter fragments in which BES1/RD26-binding sites were mutated. BES1 and RD26 were expressed in the reporter strains with pGBKT7 and pGADT7, respectively. The LacZ expression in each strain was determined by filter assays.
The raw RNA-seq reads are deposited to NCBI SRA with accession number PRJNA223275. All other data supporting the findings of this study are available within the manuscript and its supplementary files or are available from the corresponding author upon request.
How to cite this article: Ye, H. et al. RD26 mediates crosstalk between drought and brassinosteroid signalling pathways. Nat. Commun. 8, 14573 doi: 10.1038/ncomms14573 (2017).
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Supplementary Figures and Supplementary Tables
List of BR-induced genes revealed by RNA-seq. The BR-induced genes were identified by RNA-seq with 4-week-old adult plants treated with or without 1 μM BL.
List of BR-repressed genes revealed by RNA-seq. The BR-induced genes were identified in this study by RNA-seq with 4-week-old adult plants treated with or without 1 μM BL.
List of BR-induced genes revealed by microarrays. The BR-induced genes in seedling or adult plants derived from previous microarray studies. The original data were also reanalyzed as described in Methods section.
List of BR-repressed genes revealed by microarrays. The BR-repressed genes in seedling or adult plants derived from previous microarray studies . The original data were also reanalyzed as described in Methods section.
List of genes up-regulated in RD26OX transgenic plants. The genes up-regulated in RD26OX plants compared to WT were identified in this study by RNA-seq with 4-week-old adult plants without BL treatment (Fig. 2).
List of genes down-regulated in RD26OX transgenic plants. The genes down-regulated in RD26OX plants compared to WT were identified in this study by RNA-seq with 4-week-old adult plants without BL treatment (Fig. 2).
List of genes up-regulated in rd26 anac019 anac055 anac102 quadruple mutants. The genes up-regulated in rd26 anac019 anac055 anac102 quadruple mutant plants compared to WT were identified in this study by RNA-seq with 4-week-old adult plants without BL treatment (Supplementary Figure 4).
List of genes down-regulated in rd26 anac019 anac055 anac102 quadruple mutants. The genes down-regulated in rd26 anac019 anac055 anac102 quadruple mutant plants compared to WT were identified in this study by RNA-seq with 4-week-old adult plants without BL treatment (Supplementary Figure 4).
List of genes up-regulated by drought stress. Drought induced genes (combination of 2-day and 3-day dehydration treatment data) were from previous study by microarray analysis.
List of genes down-regulated by drought stress. Drought induced genes (combination of 2-day and 3-day dehydration treatment data) were from previous study by microarray analysis.
We thank Dr Eddy Yeh for help with RNA-seq analysis, Weijia Su for helping with BR and BRZ response experiments and Tadao Asami (University of Tokyo) for providing BRZ. The work is supported by grants from the NSF (IOS-1257631) and the Plant Science Institute at Iowa State University.
S.L. and P.S.S. are shareholders of Data2Bio LLC, Ames, IA, USA. The remaining authors declare no competing financial interests.
Author contributions H.Y. and Y.Y. originally conceived the project. H.Y., B.T., J.C., Z.X. and H.J. performed genetic, physiological, biochemical and gene expression studies. T.M.N. performed BiFC and gene-clustering analyses. S.L., H.-Y.L., L.L., Y.W., M.Z., Z.L. and P.S.S. conducted the RNA-seq and bioinformatics analyses. H.T. and C.C. are involved in yeast one-hybrid assays. H.G. and Y.Y. performed ChIP and reChIP experiments. M.A. and S.A. performed computational modelling. H.Y. and Y.Y. wrote the paper with contributions from most co-authors.