Ambient temperature sensing by phytochrome B (PHYB) in Arabidopsis is thought to operate mainly at night. Here we show that PHYB plays an equally critical role in temperature sensing during the daytime. In daytime thermosensing, PHYB signals primarily through the temperature-responsive transcriptional regulator PIF4, which requires the transcriptional activator HEMERA (HMR). HMR does not regulate PIF4 transcription, instead, it interacts directly with PIF4, to activate the thermoresponsive growth-relevant genes and promote warm-temperature-dependent PIF4 accumulation. A missense allele hmr-22, which carries a loss-of-function D516N mutation in HMR’s transcriptional activation domain, fails to induce the thermoresponsive genes and PIF4 accumulation. Both defects of hmr-22 could be rescued by expressing a HMR22 mutant protein fused with the transcriptional activation domain of VP16, suggesting a causal relationship between HMR-mediated activation of PIF4 target-genes and PIF4 accumulation. Together, this study reveals a daytime PHYB-mediated thermosensing mechanism, in which HMR acts as a necessary activator for PIF4-dependent induction of temperature-responsive genes and PIF4 accumulation.
Ambient growth temperature profoundly influences almost every facet of plant development and growth1. Increases in global temperature have already had dramatic impacts on plant phenology, distribution, diversity, and are expected to significantly decrease crop productivity2,3,4,5,6. A molecular understanding of how plants sense and respond to temperature becomes critical to predict the ecological impact of global temperature increases and develop new technologies to cope with climate change.
In Arabidopsis, changes in ambient temperature between 12 °C and 27 °C trigger diverse developmental, physiological, and morphological responses, including modulations in shoot and root growth, stomatal differentiation, flowering, immunity, and yield, which are collectively called thermomorphogenesis1,7,8,9,10,11,12,13. Among these, a widely used readout for thermosensing is the elongation response to warm temperatures of the embryonic stem or hypocotyl14. Hypocotyl elongation is controlled by the circadian clock and partitioned to a certain time of the day, which varies between short-day (SD) and long-day (LD) conditions15,16,17. In SD conditions, hypocotyl elongation mainly occurs at the end of night or in the dark16. By contrast, in LD, including continuous light conditions, hypocotyl elongation peaks during daytime in the light15,16,17. In accordance with the contrast in daylength-dependent rhythmic growth patterns, hypocotyl elongation is modulated by temperature changes at the distinct times in either the dark or light under SD and LD conditions, respectively18.
Ambient temperature is sensed by the red (R) and far-red (FR) photoreceptor, phytochrome B (PHYB)19,20. PHYB can be photoconverted between two relatively stable forms: the R light-absorbing inactive Pr form and the FR light-absorbing active Pfr form21,22. The active PHYB controls almost all aspects of plant development and growth, including restricting hypocotyl elongation23,24. The photoconversion by R and FR light enables phytochromes to sense changes in the ratio between R and FR light, which inform the presence of competing neighboring plants as well as the diurnal and seasonal time25,26,27, and thus to connect the environmental cues with morphological reactions or plant behaviors, such as hypocotyl elongation. The Pfr form can also be thermodynamically reverted back to Pr through a temperature-dependent process called dark- or thermo-reversion. Increases in temperature between 10 °C and 30 °C accelerate the dark-reversion rate of PHYB, leading to a reduction of the steady-state level of the active Pfr form19. This temperature-dependent biophysical property makes PHYB a thermosensor for ambient growth temperatures19,20.
Extensive studies have demonstrated that PHYB plays a critical role in regulating temperature-dependent hypocotyl growth under SD conditions. Increases in ambient temperature at night promote PHYB’s Pfr-to-Pr dark reversion that releases the inhibitory function of PHYB in hypocotyl elongation19,20. PHYB controls downstream seedling morphogenesis by regulating a group of basic helix–loop–helix (bHLH) transcriptional regulators, the phytochrome-interacting factors (PIFs)28. The PIFs belong to subfamily 15 of the bHLH protein superfamily in Arabidopsis and include eight members: PIF1, PIF3–8, and PIL1 (PIF3-like1)28,29. Different PIFs play overlapping and distinct roles in Arabidopsis seedling morphogenesis30,31. For example, hypocotyl elongation is promoted by PIF1, PIF3, PIF4, PIF5, and PIF730,31,32,33. However, thermomorphogenesis is centrally controlled by PIF49,10. High temperatures promote the expression of PIF4 at the transcriptional and posttranslational levels. PIF4 transcription is tightly regulated by the circadian clock and exhibits distinct rhythmic patterns under LD and SD conditions16,34. The transcript level of PIF4 peaks during the day in LD, but at the end of night in the SD16,18,34, which coincides with the expression of the growth-relevant PIF4 target genes, particularly genes involved in auxin synthesis and signaling16,18,35,36. During early night in SD conditions, PIF4 transcription is repressed by the evening complex components EARLY FLOWERING3 (ELF3), EARLY FLOWERING4 (ELF4), and LUX ARRHYTHMO (LUX)37. This transcriptional inhibition of PIF4 is released later at night allowing PIF4 transcripts to peak right before dawn. The transcriptional repression activity of the evening complex is dependent on PHYB and can be negatively regulated by warm temperatures16,37,38,39. Under warm temperatures, the transcript level of PIF4 is elevated at night, leading to enhanced hypocotyl elongation. At the posttranslational level, PIF4 activity and stability are regulated at night. PIF4 activity is inhibited by ELF3 and TOC1 through direct binding to PIF4’s bHLH DNA-binding domain40,41. The interaction between PIF4 and PHYB could result in phosphorylation and subsequent ubiquitin/proteasome-dependent degradation of PIF442. Warm temperatures promote PIF4 stabilization43, which depends on two antagonists for PHYB signaling, DE-ETIOLATED1 (DET1) and CONSTITUTIVE PHOTOMORPHOGENIC1 (COP1)18,44,45.
Because PHYB’s dark-reversion rate can be influenced by temperature in the light, PHYB should theoretically be able to sense temperature during daytime in LD conditions, including continuous light20. A growing body of evidence supports a thermosensory role of PHYB under LD conditions. For example, warm-temperature-dependent hypocotyl elongation in LD conditions depends on many PHYB signaling components, including PIF4, COP1, DET1, and HY518,46. However, the function of PHYB signaling in thermosensing in the light remains elusive. One major reason is that the reported temperature responses of hypocotyl elongation in LD and continuous light conditions have been inconsistent9,14,45. The minimal responses to warm temperatures under certain LD conditions have left the impression that PHYB plays only a minor role in temperature sensing during daytime45,47. In addition, most of the temperature experiments in LD conditions were performed in the white light, where the blue light photoreceptor crytochrome 1 (CRY1) strongly represses warm-temperature-dependent hypocotyl elongation48. Hence, PHYB-mediated temperature responses could also be masked by CRY1 signaling in the white light. Here, we show that the warm-temperature response in the white light is unexpectedly complex and largely influenced by the interplay between growth conditions and CRY1 signaling. To circumvent this issue, we characterized the roles of PHYB, PIFs, and HEMERA (HMR)—a PHY-specific signaling component49—under monochromatic R light, where only PHYB but not CRY1 is active. Our results demonstrate that PHYB also controls temperature sensing in the light. The daytime temperature sensing by PHYB signals through primarily PIF4 and requires HMR. This study reveals a novel PHYB-mediated temperature-signaling mechanism, in which HMR acts as an essential transcriptional activator to induce the expression of growth-relevant PIF4 target genes and PIF4 accumulation in warm temperatures.
PHYB controls thermomorphogenesis in the daytime
The first step toward understanding PHYB’s role in thermosensing under LD or continuous light conditions is to determine an optimal plant growth condition that elicits a significant response to warm temperatures. The reported temperature responses of hypocotyl elongation in LD or continuous light conditions have been inconsistent—the warm-temperature-induced increase in hypocotyl length ranged from 4.7-40 to merely 0.5-fold45. These studies were performed in different experimental settings, in which key variables such as light intensity and seedling age could contribute to the discrepancies seen in the temperature response. In addition, most of the studies were performed in the white light, where both phytochromes and the blue light photoreceptor CRY1 are activated. The presence of CRY1, which strongly inhibits the warm-temperature response48, could mask PHYB’s thermosensory role. To search for a satisfying condition, we devised experiments to determine the variables that could influence the warm-temperature response in the white light. We first examined the hypocotyl responses of Col-0 and cry1 grown for 4 days at 21 °C and 27 °C under different intensities of white light: 100, 40, and 10 μmol m−2 s−1. The results of these experiments showed that the warm-temperature response could be altered dramatically under different light intensities: the response declined with increases of light intensity (Fig. 1). The percentage of increase in hypocotyl length at 27 °C vs. 21 °C was 147% in 10 μmol m−2 s−1, 75% in 40 μmol m−2 s−1, and only 21% in 100 μmol m−2 s−1 white light (Fig. 1). More interestingly, the reduced temperature responses in 40 and 100 μmol m−2 s−1 white light were mainly due to CRY1, because the cry1 mutant showed 322% and 131% increases in the hypocotyl response under 40 and 100 μmol m−2 s−1 white light, respectively. These results indicate that CRY1 plays a major role in repressing the warm-temperature response in the white light. However, the role of CRY1 was unexpectedly reversed in 10 μmol m−2 s−1 white light, where cry1 was less responsive to the warm temperature compared with Col-0 (Fig. 1), indicating that CRY1 facilitates the warm-temperature response under this low-light condition. The latter result suggests that CRY1’s role in temperature sensing depends on growth conditions and it could play completely opposite roles in different light intensities. To test whether the role of CRY1 is also always determined by light intensity, we examined another commonly used growth condition in relatively high light intensity but using relatively older seedlings9,18,40,46. Col-0 and cry1 were grown in 100 μmol m−2 s−1 white light at 21 °C for 4 days and then were either transferred to 27 °C or maintained at 21 °C under the same light intensity for another 4 days before measurements. In this experimental setup, Col-0 showed a 273% increase in hypocotyl length comparing 27 °C vs. 21 °C (Fig. 1). Surprisingly, cry1 showed a reduced response of 113% (Fig. 1), suggesting that CRY1 promotes the temperature response under this high-light condition. Therefore, the role of CRY1 is not always determined by light intensity and could also be influenced by seedling’s developmental stage. Together, these results show that the temperature response in the white light can be largely influenced by light intensity and developmental stage, as well as the interplay between the growth conditions and CRY1 signaling.
To circumvent the complex effects of CRY1 on the warm-temperature response in the white light, we decided to examine PHYB’s role in temperature sensing using monochromatic R light, where only phytochromes, but not cryptochromes, are activated. To that end, we examined the hypocotyl responses of Col-0 at 21 °C and 27 °C under SD, LD, and continuous light conditions with the light periods in monochromatic R light. Under these conditions, the hypocotyl response to warm temperature was more pronounced in continuous R light (Rc) and LD conditions than that in SD in R light. Comparing 27 °C to 21 °C, hypocotyl length increased by 140 ± 18% and 140 ± 6% in Rc and LD conditions, and only 78% ± 5% in SD (Fig. 2a–d). In striking contrast, in Rc and LD conditions, the hypocotyls of phyB-9 and phyA-211/phyB-9 mutants—a double mutant of the two prominent phytochromes in Arabidopsis—increased only by less than 10% and there was no significant difference between phyB-9 and phyA-211/phyB-9, indicating that the daytime warm-temperature-dependent response in Rc and LD is controlled specifically by PHYB (Fig. 2). It is important to note that phyB-9 was recently reported to contain a second-site mutation that affects chloroplast development, and this mutation is not present in phyA-211/phyB-950. The fact that phyB-9 and phyA-211/phyB-9 showed similar temperature responses indicates that the reduction of the temperature response in phyB-9 is independent of the second-site mutation. Based on these results, we conclude that PHYB also mediates daytime thermosensing in the light.
Thermomorphogenesis requires the transactivator HMR
To further investigate how PHYB signaling transduces daytime temperature signals, we tested whether the warm-temperature-induced hypocotyl elongation response in R light requires the phytochrome-signaling component HMR. HMR participates specifically in phytochrome signaling but not CRY signaling in blue light49. We have previously shown that HMR is a transcriptional activator involved in early steps of PHYB signaling, including PHYB localization to the subnuclear photobodies and the regulation of the stability and activity of PIF1 and PIF349,51,52. To test whether HMR is involved in thermomorphogenesis, we examined the hypocotyl response of the null hmr-5 mutant in continuous light, LD, and SD conditions with monochromatic R light under 21 °C and 27 °C. To better compare the temperature response of the mutant, we normalized the relative hypocotyl length differences at 27 °C vs. 21 °C in the mutant against those in Col-0 to calculate the “relative response” for the mutant. The hmr-5 mutant retained a 39% relative response to warm temperature in SD, but only 25% and 8% relative response in LD and Rc, respectively (Fig. 2), indicating that HMR’s role in thermosensing is day-length dependent—it plays a more prominent role in temperature sensing during the day under LD and Rc conditions than at night under SD conditions. Collaborating with the data in R light, hmr-5 and hmr-22 in continuous white light almost lost the temperature response with only 2 and 4% relative responses, respectively, these phenotypes were similar to that of pif4-2 (Fig. 2e). Under this white light condition, phyB-9 and phyA-211/phyB-9 showed much reduced relative responses of 33 and 19% (Fig. 2e), supporting an important role of PHYB for thermosensing in white light. Interestingly, phyB-9 in the white light showed a greater warm-temperature response than in Rc (Fig. 2b), suggesting that the warm-temperature response in the white light is also mediated by sensors besides PHYB. Together, these results reveal that HMR is an essential signaling component for PHYB-mediated temperature sensory responses, particularly in the light.
HMR is dual targeted to the nucleus and plastids49,53. While nuclear HMR participates in PHY signaling49,51,52, plastidial HMR, also called pTAC12 (plastid transcriptionally active 12), is associated with the plastid-encoded plastid RNA polymerase (PEP) and required for chloroplast biogenesis54,55. Deficiency of the PEP initiates a plastid-to-nucleus retrograde signaling pathway to modulate nuclear gene expression56,57, such as the repression of the nuclear-encoded photosynthetic genes as well as the attenuation of the light-dependent inhibition of hypocotyl elongation58,59. Therefore, the lack of the warm-temperature-dependent hypocotyl response in hmr-5 could be due to its chloroplast defects. To test this possibility, we treated Col-0 seedlings with lincomycin—a potent inhibitor for chloroplast translation leading to the loss of the plastid-encoded core subunits of the PEP RNA polymerase56,60—and asked whether defects in the PEP and chloroplast biogenesis could alter the warm-temperature response in hypocotyl elongation. The lincomycin-treated albino Col-0 seedlings showed only a minimal effect on the temperature response with an 80% relative response (Fig. 2b). These results indicate that the insensitivity of hmr-5 to the ambient temperature fluctuation is not caused by defects in the PEP or chloroplast biogenesis, but most likely due to the lack of HMR’s function in the nucleus.
HMR participates in early PHY signaling in the nucleus as a transcriptional activator, which regulates the stability and activity of PIF1 and PIF349,52. A weak allele, hmr-22, which carries a loss-of-function D516N mutation in HMR’s acidic transcriptional activation domain (TAD), abrogates light-dependent degradation of PIF1 and PIF3 as well as the expression of PIF-regulated, growth-relevant genes52. The hmr-22 mutant exhibited reduced hypocotyl responses to warm temperatures in SD, LD, and Rc conditions with 62%, 41%, and 28% relative responses, respectively (Fig. 2). Consistent with the phenotype of hmr-5, hmr-22’s temperature responses in Rc and LD were more pronounced than those in SD (Fig. 2). Together, these results provide genetic evidence demonstrating that thermomorphogenesis requires HMR and particularly HMR’s TAD.
HMR mediates thermomorphogenesis through PIF4
It was surprising that hmr-5 and hmr-22 at 27 °C were shorter compared with Col-0, whereas at 21 °C, they were taller than Col-0 (Fig. 2)49,51,61. The long-hypocotyl phenotype of hmr at 21 °C has been explained by the accumulation of the hypocotyl growth-promoting factors, PIF1 and PIF349,51,61. In contrast, thermomorphogenesis in warm temperature is mediated by the central regulator PIF49,10. Therefore, the discrepancy of hmr’s hypocotyl phenotypes under different temperatures might be explained by the distinct PIFs that HMR exerts its functions onto. For example, hmr’s short-hypocotyl phenotype at 27 °C might reflect the specific function of HMR to PIF4. To test this hypothesis, we performed genetic experiments to determine the relationship between HMR and individual PIF1, PIF3, PIF4, and PIF5 for hypocotyl elongation at 21 °C and 27 °C. Because the previous studies of PIF functions in thermomorphogenesis were mostly performed under white light9,18,19,62, these experiments also aimed to confirm the roles of the distinct PIFs in thermomorphogenesis in monochromatic R light. We first re-examined the hypocotyl response of single pif1, pif3, pif4, and pif5 mutants under 21 °C and 27 °C (Fig. 3a, b). The pif4-2 mutant showed the least temperature response (Fig. 3a, b). However, under Rc, the pif4 mutant retained a 39% relative response (Fig. 3b), suggesting that thermomorphogenesis under monochromatic R light requires other factors besides PIF4. pif1-2 and pif5-3 were slightly hyposensitive to warm temperature with 73% and 60% relative responses, respectively, indicating that both PIF1 and PIF5 contribute to the hypocotyl thermoresponse (Fig. 3a, b). Surprisingly, pif3-7, despite being shorter than Col-0 at both 21 °C and 27 °C, showed an enhanced response to high temperature with a 132% relative response (Fig. 3b), suggesting that although PIF3 promotes hypocotyl growth, it plays a negative role in the warm-temperature response. Together, these results indicate that daytime thermosensing is mediated primarily through PIF4 with PIF1 and PIF5 playing minor roles, and that the role of PIFs in promoting hypocotyl elongation per se could be separable from those mediating the temperature response.
We then investigated whether individual PIFs were sufficient to mediate thermomorphogenesis by comparing pifq with various combinations of pif triple mutants that retain only one of the four PIFs. Among the four pif triple mutants, only pif135, which expresses PIF4, exhibited a wild-type thermoresponse, whereas the rest of the pif triple mutants behaved similarly to pifq (Fig. 3c, d). These results indicate that among the four PIFs, only PIF4 is sufficient to mediate thermomorphogenesis in Rc. Interestingly, the PIF4-dependent thermoresponse was reduced dramatically to 17% in pif135/hmr-5 and 46% in pif135/hmr-22 (Fig. 3d). These results demonstrate that the PIF4-dependent warm-temperature response requires HMR.
HMR is required for the PIF4-mediated thermosensory pathway. However, it is worth noting that hmr-5, with a relative response of 8%, was significantly more hyposensitive to warm temperature than pif4-2 with a relative response of 39% (Fig. 3a, b). In addition, the hmr-5/pif4-2 double mutant showed a relative response similar to hmr-5 (Fig. 3a, b). These results suggest that HMR participates in PIF4-dependent and PIF4-independent thermosensing pathways. Interestingly, when looking at the hmr-5 phenotype in pif4-2 background, hmr-5/pif4-2 was taller than pif4-2 at both 21 °C and 27 °C (Fig. 3b). These results indicate that the short-hypocotyl phenotype of hmr-5 at 27 °C is indeed dependent on PIF4. Therefore, we conclude that daytime thermosensing signals primarily through a HMR-dependent PIF4 pathway.
HMR facilitates PIF4 accumulation in warm temperatures
Warm temperature elevates PIF4 expression at both the transcriptional and posttranscriptional levels9,43. We first tested whether HMR was required for the accumulation of PIF4 transcripts under 27 °C in Rc, LD, and SD conditions as well as during the transition from 21 °C to 27 °C. The PIF4 transcript level was examined at the 96-h time point after stratification in Rc. Because warm-temperature-mediated induction of PIF4 is gated by the circadian clock40,63, we also determined the PIF4 levels at ZT8 (zeitgeber time) during the day in LD and ZT22 at the end of night in SD conditions, where the PIF4 transcript level and hypocotyl growth peak in the respective conditions16,18. The results of these experiments showed that the steady-state PIF4 transcript levels in hmr-5 and hmr-22 were similar to or within a twofold range compared with that in Col-0 (Fig. 4a). The PIF4 transcript level was also induced in hmr-22 during the transition from 21 °C to 27 °C similarly to that in Col-0 (Fig. 4b). These results indicate that HMR does not regulate PIF4 at the transcript level. In contrast, the steady-state protein level of PIF4 dramatically decreased in hmr-5 under Rc, LD, and SD conditions compared with that in Col-0 in the respective conditions (Fig. 4c). The level of PIF4 in hmr-22, compared with that of Col-0, remained the same in SD conditions but was reduced by 37.5 and 31.8% in Rc and LD conditions, respectively. These results are consistent with the more pronounced phenotypes of hmr-22 in Rc and LD conditions. Moreover, during the 21 °C to 27 °C transition, hmr-22 failed to accumulate PIF4 (Fig. 4d), suggesting that the TAD of HMR plays a crucial role in PIF4 accumulation, particularly during the early response to elevated temperatures. Together, these results support the conclusion that HMR and HMR’s transactivation activity are required not for warm-temperature-dependent increase in PIF4 transcript but rather specifically for the thermoresponsive PIF4 protein accumulation.
HMR interacts directly with PIF4
We have previously shown that HMR interacts directly with PIF1 and PIF3 to promote their degradation and to activate a group of growth-promoting PIF target genes52. HMR binds PIF1 and PIF3 through the active phytochrome B-binding (APB) motif, which is conserved in all PIFs64, including PIF452. Therefore, we hypothesized that HMR could regulate PIF4 through direct interaction. To test this hypothesis, we performed glutathione S-transferase (GST) pull-down assays using recombinant GST-HMR to pull down in vitro-translated HA-tagged full-length as well as a series of N- or C-terminal truncations of PIF4. These experiments showed that GST-HMR, but not GST alone, can pull down PIF4 (Fig. 4e), confirming that HMR physically interacts with PIF4 in vitro. Moreover, deleting the N-terminal region of PIF4 including amino acids 1–129 in HA-PIF4C2 abolished the interaction with HMR, and this N-terminal fragment alone in HA-PIF4N3 was sufficient to bind HMR (Fig. 4e). Deleting the APB alone in HA-PIF4C1 dramatically dampened the interaction (Fig. 4e). These results indicate that the HMR–PIF4 interaction is mainly mediated by the N-terminus of PIF4 containing the APB motif. We have also tried to detect the in vivo interaction between HMR and PIF4. However, these attempts were unsuccessful. This might be due to low levels of HMR in the nucleus in both Col-0 and the transgenic lines expressing HMR-HA51,52 or the HMR–PIF4 interaction being transient therefore making it difficult to capture.
Thermoresponsive genes are activated by HMR’s TAD
We then examined how the temperature-responsive PIF4 target genes are affected in the hmr mutants. To that end, we focused on three well-characterized warm-temperature-induced marker genes involved in the biosynthesis and signaling of the plant growth hormone auxin—YUC8, IAA19, and IAA2936. In Rc and LD conditions at 27 °C, the steady-state levels of YUC8, IAA19, and IAA29 in hmr-5 were dramatically reduced to levels similar to those in pif4-2 (Fig. 5a). However, the expression of these genes was only moderately reduced in SD (Fig. 5a). These results are consistent with the notion that HMR plays a more important role for thermosensing in LD and Rc conditions. The expression of these genes was only slightly changed in hmr-22 (Fig. 5a). However, during the 21 °C to 27 °C transition, the induction of all three marker genes was blocked in hmr-22 (Fig. 5b). The latter results indicate that the activity of HMR’s TAD is required for the activation of PIF4 target genes during the transition to warm temperatures.
Fusing VP16 TAD to HMR22 rescues its signaling functions
It was intriguing that a loss-of-function mutation of HMR’s TAD in hmr-22 could lead to defects in both the activation of PIF4 target genes as well as PIF4 accumulation. This raises the possibility that PIF4 accumulation is dependent on the activation of its target genes by HMR. To test this hypothesis and to confirm that the in vivo function of HMR relies on the activity of its TAD, we fused the transactivation domain of VP16 and an HA tag to HMRD516N (hereafter named HMR22), and asked whether HMR22-HA-VP16 could rescue the defects of HMR22. To this end, we first examined whether HMR22-HA-VP16/hmr-22 lines could rescue the hypocotyl growth defect of hmr-22 in response to warm temperature. Indeed, while expressing HMR-HA in hmr-22 rescued the relative response of hmr-22 from 27 to 100%, HMR22-HA-VP16 rescued to 75% relative response (Fig. 6a, b). Consistent with the hypocotyl phenotype, the expression of the three thermoresponsive PIF4 target genes in HMR22-HA-VP16/hmr-22 was also elevated to their levels in HMR-HA/hmr-22 (Fig. 6c). These data indicate that the transactivation domain of VP16 can rescue the defect of HMR’s TAD, supporting the notion that the thermoresponsive genes are activated by HMR’s TAD in vivo. More interestingly, during the 21 °C to 27 °C transition, the HMR22-HA-VP16/hmr-22 line also largely rescued hmr-22’s defect in PIF4 accumulation (Fig. 6d). These results provide genetic evidence that PIF4 accumulation in warm temperature is dependent on HMR and particularly HMR’s transactivation activity in vivo.
Plants are more likely to encounter higher temperatures during the daytime in the light. Therefore, the understanding of daytime temperature sensing at the molecular level will be critical in deciphering how plants sense, respond, and adapt to higher temperatures. However, if and how PHYB signaling participates in temperature sensing in the light remains elusive. We show here that the complex temperature responses in the white light, mainly contributed by the interplay between growth conditions and CRY1 signaling (Fig. 1), have made it difficult to discern the function of PHYB in thermonsensing. Using monochromatic R light conditions specifically activating the phytochrome photoreceptors, we show that PHYB controls the daytime hypocotyl elongation response to warm temperatures in LD and continuous light conditions. Daytime temperature sensing requires the phytochrome-specific signaling component HMR and its transcriptional activation function for regulating the activity and stability of the central temperature-responsive transcription factor PIF4. We propose that while PHYB mediates night-time temperature responses in SD conditions by controlling PIF4 transcription through the evening complex37,38,39, PHYB controls daytime temperature-dependent hypocotyl elongation in the light mainly through the regulation of the activity and stability of PIF4 by HMR.
Hypocotyl elongation occurs during the daytime or in the light under LD conditions and before dawn or in the dark in SD15,16,18. The main difference between the LD and SD hypocotyl elongation is that daytime hypocotyl elongation is regulated directly by active PHYB, whereas night-time elongation in SD is indirectly controlled by PHYB through the regulation of PIF4 transcription via the evening complex. Therefore, the LD and SD hypocotyl elongation represents two distinct growth modes—PHYB-dependent growth in the light and PHYB-independent growth in the dark, respectively. Our results demonstrate that PHYB plays an equally important role in daytime temperature sensing (Fig. 2). PHYB’s thermosensory role during daytime has been poorly recognized, largely because of the inconsistent hypocotyl responses to warm temperatures in LD conditions. The minimal temperature response in hypocotyl elongation under certain LD conditions in the white light45 has led to the notion that PHYB’s temperature-dependent dark-reversion rate operates primarily in the dark by influencing how fast the active PHYB diminishes at night19,47,65. However, an acceleration in dark-reversion rate, similar to an increase of FR light, is expected to tip the balance of the Pfr to Pr ratio as well as increase the processivity or the cycling rate between Pr and Pfr of PHYB in the light20. Therefore, PHYB should theoretically be able to perceive ambient temperature changes in the light20. In support of this conclusion, we provide genetic evidence that in monochromatic R light, the warm-temperature-dependent hypocotyl response is more pronounced in Rc and LD than SD conditions, and the temperature response in Rc and LD conditions is PHYB-dependent (Fig. 2). These results, combined with the fact that the temperature-dependent hypocotyl elongation occurs during daytime in the light15,16,17,18, indicate that PHYB controls thermomorphogenesis in the light. Our results also show that PHYB plays a major role in continuous white light (Fig. 2e), although it is worth noting that under our white light condition, phyB-9 retained 33% of Col-0’s warm-temperature response, suggesting that temperature sensing in the white light must also be mediated by other sensors besides PHYB. It is also intriguing that the PHYB-dependent hypocotyl thermoresponse is masked by CRY1 under certain growth conditions but promoted under others (Fig. 1). The inhibitory role of CRY1 to the temperature responses is likely through its dominant inhibitory function on PIF448. Further investigations are needed to dissect the dynamic interactions between PHYB and CRY1 pathways in thermomorphogenesis.
Supporting a critical role of PHYB signaling in thermosensing in the light, we showed that daytime thermosensing requires a phytochrome-specific signaling component HMR. HMR contributes more significantly to thermonsensing in Rc and LD than in SD conditions (Fig. 2). This is consistent with the published results that HMR’s function is PHYB-dependent and is required for hypocotyl growth in the light but not in the dark49,51. Other signaling components have also been shown to exert significant roles only under LD or SD conditions. For example, HY5 plays a more pronounced role in thermorsensing in LD conditions45,46, whereas ELF3 is only involved in SD conditions18. Together, our results, in combination with the published data, strongly support the notion that PHYB controls thermoresponsive hypocotyl elongation under LD and SD through distinct mechanisms. We propose that daytime PHYB-mediated thermosensing is mainly through the regulation of the activity and stability of PIF4 through HMR.
A central mechanism underlying thermomorphogenesis in both LD and SD conditions is through the regulation of the central temperature-responsive transcriptional regulator PIF4 and the activation of PIF4-dependent auxin biosynthetic and signaling genes, including YUC8, IAA19, and IAA299,10,18,36. This study reveals that the PIF4-mediated thermosensing depends on HMR. This conclusion is solidly supported by the genetic evidence that both hmr-5 and hmr-22 are defective in the warm-temperature-dependent hypocotyl response (Fig. 2). Knocking out PIF1, PIF3, and PIF5, with only PIF4 present, the PIF4-dependent thermoresponse in pif135 was abolished in the pif135/hmr-5 mutant, demonstrating that the function of PIF4 in thermomorphogenesis depends on HMR (Fig. 3c). Our results show that HMR regulates PIF4 not at the transcript level but rather at the posttranslational level by controlling the expression of the temperature-responsive PIF4 target genes and PIF4 accumulation. HMR is a transcriptional activator interacting directly with PIF1 and PIF352. It has been shown that HMR’s acidic TAD is responsible for the activation of PIF-regulated, growth-relevant genes as well as the degradation of PIF1 and PIF3 in the light at 21 °C52. Here, we show that HMR interacts with PIF4 in vitro through PIF4’s N-terminal region (Fig. 4e). We were not able to detect in vivo HMR–PIF4 interaction by immunoprecipitation, which might be due to low levels of HMR in the nucleus or the dynamic nature of the interaction. However, our results provide genetic evidence that defects in the transactivation function of HMR’s TAD in hmr-22 impair the warm-temperature-dependent induction of PIF4 target genes (Fig. 5b) and PIF4 accumulation (Fig. 4d). More interestingly, fusing the transactivation domain of VP16 to HMR22 rescued both defects of hmr-22 (Fig. 6c, d), indicating a causal relationship between the activation of the temperature-responsive genes by HMR and PIF4 accumulation. It is still unclear how the activity of HMR’s TAD can stabilize PIF4. One possibility is that the TAD of HMR facilitates the formation of the preinitiation complex, which helps to prevent PIF4 from degradation by the ubiquitin–proteasome pathway. PIF4 degradation is mediated by CULLIN3-based E3 ubiquitin ligases with BLADE-ON-PETIOLE (BOP) 1 and 2 as the substrate recognition subunit66. Mutants of the BOP genes showed an enhanced hypocotyl response to warm temperature66. One possibility is that HMR’s TAD function blocks PIF4 from the BOP-dependent PIF4 degradation. Warm-temperature-dependent PIF4 accumulation also depends on DET1 and COP1, both of which are also required for the induction of PIF4 target genes18,44,45. HMR could work with DET1 and COP1 in promoting PIF4 accumulation in higher temperatures.
In contrast to the white light conditions, where thermomorphogenesis relies almost entirely on PIF49,18,62, in R light, the hypocotyl response to warm temperature also depends on at least PIF1 and PIF5 (Fig. 3a, b). Interestingly, PIF3, albeit its role in promoting hypocotyl elongation, negatively regulates the hypocotyl response to warm temperature (Fig. 3a, b). Our genetic data indicate that HMR participates in both PIF4-dependent and PIF4-independent pathways in thermomorphogenesis, because both hmr-5 and hmr-5/pif4 were more hyposensitive to warm temperatures than pif4 (Fig. 3a, b). Given that HMR interacts with all PIFs52, these data might suggest that HMR could also regulate PIF1 and PIF5 in thermosensing.
It is intriguing that HMR showed opposite effects to the stability of PIF3 and PIF4. The TAD of HMR promotes PIF3 degradation but PIF4 accumulation (Fig. 4d)52. These distinct functions of HMR on the stability of PIF3 and PIF4 provide an explanation for the contrasting phenotypes of the hmr mutants under 21 °C and 27 °C: the long-hypocotyl phenotype of hmr mutants at 21 °C could be mainly due to the accumulation of PIF352, whereas the short-hypocotyl phenotype at 27 °C is caused by the defect in PIF4 accumulation (Fig. 3a). Supporting these conclusions, in the pif4 background, the hmr-5/pif4 double mutant became taller than pif4 (Fig. 3a), demonstrating that the short-hypocotyl phenotype of hmr-5 in warm temperatures is PIF4-dependent. Therefore, although HMR interacts with PIF3 and PIF4, and both of PIF3 and PIF4 are regulated by HMR’s TAD, the modes of action of HMR on PIF3 and PIF4 stability seem to be different. This discrepancy may be explained by the distinct degradation mechanisms of PIF3 and PIF4. For example, the degradation of PIF3, but not PIF4, is mediated by the carboxy-terminal signaling output module of PHYB61. PIF3 degradation is mediated by the Cullin3-LRB [(Light-Response Bric-a-Brack/Tramtrack/Broad (BTB))] and Cullin1-EBF (EIN3-binding F box protein) E3 ubiquitin ligases67,68, whereas PIF4 degradation is mediated by the Cullin3-BOP E3 ubiquitin ligases66. Further work will be focused on elucidating the mechanistic links between HMR’s TAD to the regulation of PIF3 and PIF4 stability.
HMR is dual targeted to plastids and the nucleus49,53. The plastidial HMR, also called pTAC12, is an essential component of the PEP and is required for the induction of the plastid-encoded photosynthetic genes54. Because phytochrome signaling in the nucleus can be controlled by chloroplast-to-nucleus or retrograde signals, particularly from the activity of the PEP57, one challenge in defining HMR’s function is to dissect the contributions of the nuclear and plastidial HMR. Our results show that hypocotyl elongation in warm temperatures was intact when plastid translation was inhibited by lincomycin (Fig. 2a). Because a major effect of lincomycin is to eliminate the expression of the core subunits of the PEP, which triggers the GUN signaling57, our results indicate that the hypocotyl response to warm temperatures is not influenced by the loss of the PEP or GUN signaling. Therefore, the temperature phenotype of hmr is due to defects of the nuclear HMR. These results are consistent with our previous findings that the hypocotyl phenotype of hmr at 21 °C is caused by PIF1 and PIF3 accumulation in the nucleus, which is separable from the chloroplast defects52, and HMR-regulated, growth-relevant genes are not regulated by retrograde signaling53. Together, these results provide genetic evidence that reveals HMR as an essential regulator for the nuclear PHYB- and PIF4-mediated thermomorphogenesis mechanism in the light.
Photobodies are PHYB-containing light-sensory subnuclear domains that are associated with early signaling events, such as the regulation of PIF3 degradation61,65,69,70,71,72. The biogenesis of photobodies is regulated directly by light quality and quantity, and therefore is determined by the Pfr form of PHYB73,74. In SD conditions, PHYB could regulate the evening complex and PIF4 transcription through the photobodies20,69. Photobodies function to stabilize the Pfr form of PHYB, therefore inhibiting PIF4 transcription in the dark65,75,76. Also, photobodies could directly contribute to PHYB’s function in the regulation of the evening complex, because the evening complex components are constituents of the photobodies77, and the evening complex and PHYB bind to shared genome-wide gene-regulatory sites38. During the daytime, the morphology, including size and number, of photobodies is regulated by light and temperature20,73]. HMR was identified as a light-signaling component required for the formation of large photobodies49. Given the critical function of HMR in thermomorphogenesis, this study provides genetic evidence supporting a role of photobodies in thermosensing in the daytime, which is consistent with the dynamic changes of photobody morphology under different temperatures20.
In conclusion, this study demonstrates a thermosensing role of PHYB in the daytime. We have identified HMR as an essential transcription activator in thermomorphogenesis. Our results support a novel PHYB-mediated temperature-signaling mechanism, in which HMR’s TAD facilitates the activation of thermoresponsive PIF4 target genes as well as PIF4 accumulation. Future investigations will focus on understanding the mechanistic link between the activity of HMR’s TAD and PIF4 accumulation, as well as the interaction between PHYB and CRY1 signaling in thermomorphogenesis in the white light.
Plant materials and growth conditions
The Columbia ecotype (Col-0) of Arabidopsis was used throughout this study. The phyB-9, phyA-211/phyB-9, hmr-5, and hmr-22 mutants, as well as transgenic lines HMR-HA/hmr-22 and HMR22-HA-VP16/hmr-22 were previously described52. Because hmr-5 is albino and seedling lethal, homozygous hmr-5 seedlings used in this study were from segregating populations. Single, triple, and quadruple pif mutants, including pif1-2 (SALK_072677), pif3-3 (CS66042), pif4-2 (SAIL_1288_E07), pif5-3 (SALK_087012), pif134 (CS66500), pif135 (CS66047), pif145 (CS68095), pif345 (CS66048), and pifq were previously described30 and obtained from Arabidopsis Biological Resource Center. The cry1 mutant was reported as hy4-B10478. Seeds were surface sterilized51 and plated on half-strength Murashige and Skoog media with Gamborg’s vitamins (MSP0506, Caisson Laboratories, North Logan, UT, USA), 0.5 mM MES (pH 5.7), and 0.8% (w/v) agar (A038, Caisson Laboratories, North Logan, UT, USA). For lincomycin treatments, media were supplemented with 220 µg/ml lincomycin hydrochloride (L2774, Sigma-Aldrich). Seeds were stratified in the dark at 4 ˚C for 5 days before treatment of specific light and temperature in an LED chamber (Percival Scientific). R light was kept at 10 μmol m−2 s−1 for Rc, SD (8 h day/16 h night), or LD (16 h day/8 h night) conditions. Fluence rates of light were measured using an Apogee PS200 spectroradiometer (Apogee Instruments Inc., Logan, UT, USA).
Seedlings were scanned using an Epson Perfection V700 photo scanner, and at least 30 hypocotyls were measured for each genotype and treatment using NIH ImageJ software (http://rsb.info.nih.gov/nih-image/).
Protein extraction and immunoblots
For total protein extraction, Arabidopsis seedlings were harvested and ground using a Mini-Beadbeater-24 (BioSpec Products, Inc.) in three volumes (mg/µL) of extraction buffer containing 100 mM Tris-Cl pH 7.5, 100 mM NaCl, 5 mM EDTA, 1% SDS, 5 mM DTT, 10 mM β-mercaptoethanol, 40 µM MG115 (Sigma-Aldrich), 40 µM MG132 (Sigma-Aldrich), 1× phosphatase inhibitor cocktail 3 (Sigma-Aldrich), 1× EDTA-free protease inhibitor cocktail (Roche), and 0.01% bromophenol blue. Samples were immediately boiled for 10 min and centrifuged at 16,000×g for 10 min. Proteins in the supernatant were separated by SDS-PAGE, transferred to nitrocellulose membranes, probed with the indicated primary antibodies, and then incubated with horseradish peroxidase-conjugated anti-goat, anti-mouse, or anti-rabbit secondary antibodies (Bio-Rad). Primary antibodies, including monoclonal mouse anti-HA antibodies (Sigma-Aldrich, H3663), polyclonal goat anti-HA antibodies (Genscript, A00168), polyclonal rabbit anti-HMR antibodies (homemade), polyclonal rabbit anti-PIF4 antibodies (Agrisera, AS 12 1860), and polyclonal rabbit anti-RPN6 antibodies (Enzo Life Sciences, BML-PW8370-0100) were used at 1:1000 dilution. Signals were detected by chemiluminescence using a SuperSignal kit (ThermoFisher Scientific).
RNA extraction and quantitative reverse transcription-PCR
Seedlings for RNA extraction were collected, frozen in liquid nitrogen, and stored at −80 °C before processing. Samples were ground in liquid nitrogen, and RNA was extracted using the Quick-RNA MiniPrep kit with on-column DNase I digestion (Zymo Research). cDNA synthesis was performed with the Superscript II First Strand cDNA Synthesis Kit (ThermoFisher Scientific). For qRT-PCR, cDNA was mixed with iQ SYBR Green Supermix (Bio-Rad) and primers (Supplementary Table 1). qRT-PCR reactions were performed in triplicate with a Bio-Rad CFX Connect Real-Time PCR Detection System.
To make the bait vector for GST pull-down assays, the full-length coding sequence of HMR was inserted into EcoRI and PstI sites of pET42b (Novagen). To make the prey vectors, sequences encoding PIF4 full length (amino acids 1–430) and fragments (amino acids 1–335, 1–249, 1–129, 54–430, 130–430, and 250–430) were inserted into EcoRI and XmaI sites of pCMX-PL2-NterHA. All the primers used for making constructs are listed in Supplementary Table 2.
GST pull-down assays
Bait proteins (GST and GST-HMR) were expressed in the E. coli BL21 (DE3) strain. Cells were harvested by centrifugation, and the pellet was resuspended in E buffer containing 50 mM Tris-Cl (pH 7.5), 100 mM NaCl, 1 mM EDTA, 1 mM EGTA, 1% DMSO, 2 mM DTT, and bacterial protease inhibitor cocktail (Sigma-Aldrich). All subsequent purification and binding steps were carried out at 4 °C. Cells were lysed by French press, and the lysate was centrifuged at 13,000×g for 20 min. Proteins were then precipitated with 3.3 M ammonium sulfate and incubated for 4 h at 4 °C. After centrifugation at 10,000×g for 30 min, protein pellets were resuspended in E buffer. Insoluble protein was removed by centrifugation at 13,000×g for 1 h, and the supernatant was dialyzed against E buffer overnight at 4 °C.
To immobilize bait proteins, protein extracts were incubated with glutathione Sepharose beads (GE Healthcare) equilibrated in E buffer for 2 h, and then beads were washed four times in E buffer supplemented with 0.1% Nonidet P-40. HA-tagged prey proteins were produced in vitro using the TNT T7-Coupled Reticulocyte Lysate System (Promega) according to the manufacturer’s protocol, and with the above-mentioned plasmids52. TNT products were then diluted in E buffer with 0.1% Nonidet P-40 and incubated with bead-immobilized bait proteins at 4 °C for 2 h. After binding, beads were washed four times in E buffer with 0.1% Nonidet P-40, and then protein was eluted by boiling in 1× Laemmli sample buffer. Bound proteins were separated by SDS-PAGE, and prey proteins were detected with immunoblots using polyclonal goat anti-HA antibodies (Genescript). Bait proteins were visualized by staining SDS-PAGE gels with Coomassie Brilliant blue.
Further information on experimental design is available in the Nature Research Reporting Summary linked to this article.
Arabidopsis mutants and transgenic lines, as well as plasmids generated during the current study are available from the corresponding author on reasonable request. The source data of the gels and immunoblots in Figs. 4c–e and 6d as well as the source data underlying Figs. 1, 2b, 2d, 2e, 3b, 3d, 4a, b, 51-b, and 6b, c are provided in the Source Data file.
Quint, M. et al. Molecular and genetic control of plant thermomorphogenesis. Nat. Plants 2, 15190 (2016).
Fitter, A. H. & Fitter, R. S. R. Rapid changes in flowering time in British plants. Science 296, 1689–1691 (2002).
Thuiller, W., Lavorel, S., Araújo, M. B., Sykes, M. T. & Prentice, I. C. Climate change threats to plant diversity in Europe. Proc. Natl. Acad. Sci. USA 102, 8245–8250 (2005).
Willis, C. G., Ruhfel, B., Primack, R. B., Miller-Rushing, A. J. & Davis, C. C. Phylogenetic patterns of species loss in Thoreau’s woods are driven by climate change. Proc. Natl Acad. Sci. USA 105, 17029–17033 (2008).
Nicotra, A. B. et al. Plant phenotypic plasticity in a changing climate. Trends Plant. Sci. 15, 684–692 (2010).
Bita, C. E. & Gerats, T. Plant tolerance to high temperature in a changing environment: scientific fundamentals and production of heat stress-tolerant crops. Front. Plant Sci. 4, 273 (2013).
Blázquez, M. A., Ahn, J. H. & Weigel, D. A thermosensory pathway controlling flowering time in Arabidopsis thaliana. Nat. Genet. 33, 168–171 (2003).
Yang, S. & Hua, J. A haplotype-specific Resistance gene regulated by BONZAI1 mediates temperature-dependent growth control in Arabidopsis. Plant Cell 16, 1060–1071 (2004).
Koini, M. A. et al. High temperature-mediated adaptations in plant architecture require the bHLH transcription factor PIF4. Curr. Biol. 19, 408–413 (2009).
Kumar, S. V. et al. Transcription factor PIF4 controls the thermosensory activation of flowering. Nature 484, 242–245 (2012).
Crawford, A. J., McLachlan, D. H., Hetherington, A. M. & Franklin, K. A. High temperature exposure increases plant cooling capacity. Curr. Biol. 22, R396–R397 (2012).
Ibañez, C. et al. Ambient temperature and genotype differentially affect developmental and phenotypic plasticity in Arabidopsis thaliana. BMC Plant Biol. 17, 114 (2017).
Legris, M., Nieto, C., Sellaro, R., Prat, S. & Casal, J. J. Perception and signalling of light and temperature cues in plants. Plant J. 90, 683–697 (2017).
Gray, W. M., Ostin, A., Sandberg, G., Romano, C. P. & Estelle, M. High temperature promotes auxin-mediated hypocotyl elongation in Arabidopsis. Proc. Natl Acad. Sci. USA 95, 7197–7202 (1998).
Dowson-Day, M. J. & Millar, A. J. Circadian dysfunction causes aberrant hypocotyl elongation patterns in Arabidopsis. Plant J. 17, 63–71 (1999).
Nozue, K. et al. Rhythmic growth explained by coincidence between internal and external cues. Nature 448, 358–361 (2007).
Michael, T. P. et al. A morning-specific phytohormone gene expression program underlying rhythmic plant growth. PLoS Biol. 6, e225 (2008).
Park, Y.-J., Lee, H.-J., Ha, J.-H., Kim, J. Y. & Park, C.-M. COP1 conveys warm temperature information to hypocotyl thermomorphogenesis. New Phytol. 215, 269–280 (2017).
Jung, J.-H. et al. Phytochromes function as thermosensors in Arabidopsis. Science 354, 886–889 (2016).
Legris, M. et al. Phytochrome B integrates light and temperature signals in Arabidopsis. Science 354, 897–900 (2016).
Rockwell, N. C., Su, Y. S. & Lagarias, J. C. Phytochrome structure and signaling mechanisms. Annu. Rev. Plant. Biol. 57, 837–858 (2006).
Burgie, E. S. & Vierstra, R. D. Phytochromes: an atomic perspective on photoactivation and signaling. Plant Cell 26, 4568–4583 (2014).
Reed, J. W., Nagpal, P., Poole, D. S., Furuya, M. & Chory, J. Mutations in the gene for the red/far-red light receptor phytochrome B alter cell elongation and physiological responses throughout Arabidopsis development. Plant Cell 5, 147–157 (1993).
Chen, M., Chory, J. & Fankhauser, C. Light signal transduction in higher plants. Annu. Rev. Genet. 38, 87–117 (2004).
Salter, M. G., Franklin, K. A. & Whitelam, G. C. Gating of the rapid shade-avoidance response by the circadian clock in plants. Nature 426, 680–683 (2003).
Tao, Y. et al. Rapid synthesis of auxin via a new tryptophan-dependent pathway is required for shade avoidance in plants. Cell 133, 164–176 (2008).
Franklin, K. A. & Whitelam, G. C. Light-quality regulation of freezing tolerance in Arabidopsis thaliana. Nat. Genet. 39, 1410–1413 (2007).
Leivar, P. & Quail, P. H. PIFs: pivotal components in a cellular signaling hub. Trends Plant. Sci. 16, 19–28 (2011).
Luo, Q. et al. COP1 and phyB Physically Interact with PIL1 to Regulate Its Stability and Photomorphogenic Development in Arabidopsis. Plant Cell 26, 2441–2456 (2014).
Leivar, P. et al. Multiple phytochrome-interacting bHLH transcription factors repress premature seedling photomorphogenesis in darkness. Curr. Biol. 18, 1815–1823 (2008).
Shin, J. et al. Phytochromes promote seedling light responses by inhibiting four negatively-acting phytochrome-interacting factors. Proc. Natl Acad. Sci. USA 106, 7660–7665 (2009).
Li, L. et al. Linking photoreceptor excitation to changes in plant architecture. Genes Dev. 26, 785–790 (2012).
Procko, C. et al. The epidermis coordinates auxin-induced stem growth in response to shade. Genes Dev. 30, 1529–1541 (2016).
Yamashino, T. et al. A link between circadian-controlled bHLH factors and the APRR1/TOC1 quintet in Arabidopsis thaliana. Plant Cell Physiol. 44, 619–629 (2003).
Covington, M. F. & Harmer, S. L. The circadian clock regulates auxin signaling and responses in Arabidopsis. PLoS Biol. 5, e222 (2007).
Franklin, K. A. et al. Phytochrome-interacting factor 4 (PIF4) regulates auxin biosynthesis at high temperature. Proc. Natl Acad. Sci. USA 108, 20231–20235 (2011).
Nusinow, D. A. et al. The ELF4-ELF3-LUX complex links the circadian clock to diurnal control of hypocotyl growth. Nature 475, 398–402 (2011).
Ezer, D. et al. The evening complex coordinates environmental and endogenous signals in Arabidopsis. Nat. Plants 3, 17087 (2017).
Box, M. S. et al. ELF3 controls thermoresponsive growth in Arabidopsis. Curr. Biol. 25, 194–199 (2015).
Zhu, J.-Y., Oh, E., Wang, T. & Wang, Z.-Y. TOC1-PIF4 interaction mediates the circadian gating of thermoresponsive growth in Arabidopsis. Nat. Commun. 7, 13692 (2016).
Nieto, C., Lopez-Salmeron, V., Daviere, J. M. & Prat, S. ELF3-PIF4 interaction regulates plant growth independently of the evening complex. Curr. Biol. 25, 187–193 (2015).
Lorrain, S., Allen, T., Duek, P. D., Whitelam, G. C. & Fankhauser, C. Phytochrome-mediated inhibition of shade avoidance involves degradation of growth-promoting bHLH transcription factors. Plant J. 53, 312–323 (2008).
Foreman, J. et al. Light receptor action is critical for maintaining plant biomass at warm ambient temperatures. Plant J. 65, 441–452 (2011).
Dong, J. et al. Arabidopsis DE-ETIOLATED1 represses photomorphogenesis by positively regulating phytochrome-interacting factors in the dark. Plant Cell 26, 3630–3645 (2014).
Gangappa, S. N. & Kumar, S. V. DET1 and HY5 control PIF4-mediated thermosensory elongation growth through distinct mechanisms. Cell Rep. 18, 344–351 (2017).
Delker, C. et al. The DET1-COP1-HY5 pathway constitutes a multipurpose signaling module regulating plant photomorphogenesis and thermomorphogenesis. Cell Rep. 9, 1983–1989 (2014).
Cortijo, S. et al. Transcriptional regulation of the ambient temperature response by H2A.Z nucleosomes and HSF1 transcription factors in Arabidopsis. Mol. Plant 10, 1258–1273 (2017).
Ma, D. et al. Cryptochrome 1 interacts with PIF4 to regulate high temperature-mediated hypocotyl elongation in response to blue light. Proc. Natl Acad. Sci. 113, 224–229 (2016).
Chen, M. et al. Arabidopsis HEMERA/pTAC12 initiates photomorphogenesis by phytochromes. Cell 141, 1230–1240 (2010).
Yoshida, Y. et al. The Arabidopsis phyB-9 mutant has a second-site mutation in the VENOSA4 gene that alters chloroplast size, photosynthetic traits, and leaf growth. Plant Physiol. 178, 3–6 (2018).
Galvao, R. M. et al. Photoactivated phytochromes interact with HEMERA and promote its accumulation to establish photomorphogenesis in Arabidopsis. Genes Dev. 26, 1851–1863 (2012).
Qiu, Y. et al. HEMERA couples the proteolysis and transcriptional activity of PHYTOCHROME INTERACTING FACTORs in Arabidopsis photomorphogenesis. Plant Cell 27, 1409–1427 (2015).
Nevarez, P. A. et al. Mechanism of dual targeting of the phytochrome signaling component HEMERA/pTAC12 to plastids and the nucleus. Plant Physiol. 173, 1953–1966 (2017).
Pfalz, J., Liere, K., Kandlbinder, A., Dietz, K. J. & Oelmuller, R. pTAC2, -6, and -12 are components of the transcriptionally active plastid chromosome that are required for plastid gene expression. Plant Cell 18, 176–197 (2006).
Pfalz, J. et al. ZmpTAC12 binds single-stranded nucleic acids and is essential for accumulation of the plastid-encoded polymerase complex in maize. New Phytol. 206, 1024–1037 (2015).
Koussevitzky, S. et al. Signals from chloroplasts converge to regulate nuclear gene expression. Science 316, 715–719 (2007).
Woodson, J. D., Perez-Ruiz, J. M., Schmitz, R. J., Ecker, J. R. & Chory, J. Sigma factor-mediated plastid retrograde signals control nuclear gene expression. Plant J. 73, 1–13 (2012).
Martín, G. et al. Phytochrome and retrograde signalling pathways converge to antagonistically regulate a light-induced transcriptional network. Nat. Commun. 7, 11431 (2016).
Oh, S. & Montgomery, B. L. Phytochrome-induced SIG2 expression contributes to photoregulation of phytochrome signalling and photomorphogenesis in Arabidopsis thaliana. J. Exp. Bot. 64, 5457–5472 (2013).
Nott, A., Jung, H.-S., Koussevitzky, S. & Chory, J. Plastid-to-nucleus retrograde signaling. Annu. Rev. Plant. Biol. 57, 739–759 (2006).
Qiu, Y. et al. Mechanism of early light signaling by the carboxy-terminal output module of Arabidopsis phytochrome B. Nat. Commun. 8, 1905 (2017).
Stavang, J. A. et al. Hormonal regulation of temperature-induced growth in Arabidopsis. Plant J. 60, 589–601 (2009).
Mizuno, T. et al. Ambient temperature signal feeds into the circadian clock transcriptional circuitry through the EC night-time repressor in Arabidopsis thaliana. Plant Cell Physiol. 55, 958–976 (2014).
Khanna, R. et al. A novel molecular recognition motif necessary for targeting photoactivated phytochrome signaling to specific basic helix-loop-helix transcription factors. Plant Cell 16, 3033–3044 (2004).
Van Buskirk, E. K., Reddy, A. K., Nagatani, A. & Chen, M. Photobody localization of phytochrome B is tightly correlated with prolonged and light-dependent inhibition of hypocotyl elongation in the dark. Plant Physiol. 165, 595–607 (2014).
Zhang, B. et al. BLADE-ON-PETIOLE proteins act in an E3 ubiquitin ligase complex to regulate PHYTOCHROME INTERACTING FACTOR 4 abundance. eLife 6, e26759 (2017). https://doi.org/10.7554/eLife.26759
Ni, W. et al. A mutually assured destruction mechanism attenuates light signaling in Arabidopsis. Science 344, 1160–1164 (2014).
Dong, J. et al. Light-dependent degradation of PIF3 by SCFEBF1/2 promotes a photomorphogenic response in Arabidopsis. Curr. Biol. 27, 2420–2430.e6 (2017).
Van Buskirk, E. K., Decker, P. V. & Chen, M. Photobodies in light signaling. Plant Physiol. 158, 52–60 (2012).
Yamaguchi, R., Nakamura, M., Mochizuki, N., Kay, S. A. & Nagatani, A. Light-dependent translocation of a phytochrome B-GFP fusion protein to the nucleus in transgenic Arabidopsis. J. Cell. Biol. 145, 437–445 (1999).
Kircher, S. et al. Nucleocytoplasmic partitioning of the plant photoreceptors phytochrome A, B, C, D, and E is regulated differentially by light and exhibits a diurnal rhythm. Plant Cell 14, 1541–1555 (2002).
Bauer, D. et al. Constitutive photomorphogenesis 1 and multiple photoreceptors control degradation of phytochrome interacting factor 3, a transcription factor required for light signaling in Arabidopsis. Plant Cell 16, 1433–1445 (2004).
Chen, M., Schwab, R. & Chory, J. Characterization of the requirements for localization of phytochrome B to nuclear bodies. Proc. Natl Acad. Sci. USA 100, 14493–14498 (2003).
Klose, C. et al. Systematic analysis of how phytochrome B dimerization determines its specificity. Nat. Plants 1, 15090 (2015).
Huang, H. et al. PCH1 integrates circadian and light-signaling pathways to control photoperiod-responsive growth in Arabidopsis. eLife 5, e13292 (2016).
Enderle, B. et al. PCH1 and PCHL promote photomorphogenesis in plants by controlling phytochrome B dark reversion. Nat. Commun. 8, 2221 (2017).
Huang, H. et al. Identification of evening complex associated proteins in Arabidopsis by affinity purification and mass spectrometry. Mol. Cell. Proteom. 15, 201–217 (2016).
Bruggemann, E., Handwerger, K., Essex, C. & Storz, G. Analysis of fast neutron-generated mutants at the Arabidopsis thaliana HY4 locus. Plant J. 10, 755–760 (1996).
We thank Drs. Peter Quail (UC Berkeley) and Chentao Lin (UC Los Angeles) for kindly providing the pifq and cry1 mutants, respectively. We thank Dr. Chan Yul Yoo, Dr. Keunhwa Kim, and Joseph Hahm for their critical comments and suggestions regarding the manuscript. This work was supported by grant R01GM087388 from the National Institute of General Medical Sciences to M.C.
The authors declare no competing interests.
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Qiu, Y., Li, M., Kim, R.J. et al. Daytime temperature is sensed by phytochrome B in Arabidopsis through a transcriptional activator HEMERA. Nat Commun 10, 140 (2019). https://doi.org/10.1038/s41467-018-08059-z
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