Skip to main content
PMC home page
Frontiers in Plant Science logoLink to Frontiers in Plant Science
. 2013 Oct 30;4:440. doi: 10.3389/fpls.2013.00440

Overexpression of the Mg-chelatase H subunit in guard cells confers drought tolerance via promotion of stomatal closure in Arabidopsis thaliana

Tomo Tsuzuki 1, Koji Takahashi 1, Masakazu Tomiyama 1, Shin-ichiro Inoue 1, Toshinori Kinoshita 1,2,*
PMCID: PMC3812566  PMID: 24198823

Abstract

The Mg-chelatase H subunit (CHLH) has been shown to mediate chlorophyll biosynthesis, as well as plastid-to-nucleus and abscisic acid (ABA)-mediated signaling. A recent study using a novel CHLH mutant, rtl1, indicated that CHLH specifically affects ABA-induced stomatal closure, but also that CHLH did not serve as an ABA receptor in Arabidopsis thaliana. However, the molecular mechanism by which CHLH engages in ABA-mediated signaling in guard cells remains largely unknown. In the present study, we examined CHLH function in guard cells and explored whether CHLH expression might influence stomatal aperture. Incubation of rtl1 guard cell protoplasts with ABA induced expression of the ABA-responsive genes RAB18 and RD29B, as also observed in wild-type (WT) cells, indicating that CHLH did not affect the expression of ABA-responsive genes. Earlier, ABA was reported to inhibit blue light (BL)-mediated stomatal opening, at least in part through dephosphorylating/inhibiting guard cell H+-ATPase (which drives opening). Therefore, we immunohistochemically examined the phosphorylation status of guard cell H+-ATPase. Notably, ABA inhibition of BL-induced phosphorylation of H+-ATPase was impaired in rtl1 cells, suggesting that CHLH influences not only ABA-induced stomatal closure but also inhibition of BL-mediated stomatal opening by ABA. Next, we generated CHLH-GFP-overexpressing plants using CER6 promoter, which induces gene expression in the epidermis including guard cells. CHLH-transgenic plants exhibited a closed stomata phenotype even when brightly illuminated. Moreover, plant growth experiments conducted under water-deficient conditions showed that CHLH transgenic plants were more tolerant of drought than WT plants. In summary, we show that CHLH is involved in the regulation of stomatal aperture in response to ABA, but not in ABA-induced gene expression, and that manipulation of stomatal aperture via overexpression of CHLH in guard cells improves plant drought tolerance.

Keywords: stomata, CHLH, ABA, drought tolerance, H+-ATPase, Arabidopsis

Introduction

Stomatal pores, surrounded by paired guard cells and located in the epidermis of plants, regulate gas exchange in response to both environmental and endogenous signals. Stomatal opening facilitates both transpiration and CO2 entry (to enable photosynthesis) (Shimazaki et al., 2007). Stomatal opening is triggered by blue light (BL) via activation of the plasma membrane H+-ATPase of guard cells (Assmann et al., 1985; Shimazaki et al., 1986; Kinoshita and Shimazaki, 1999). BL-induced activation of H+-ATPase involves phosphorylation of the penultimate C-terminal threonine (Thr) of the enzyme (Kinoshita and Shimazaki, 2002; Kinoshita and Hayashi, 2011).

When water is scarce, the plant hormone abscisic acid (ABA) promotes stomatal closure to prevent water loss (Schroeder et al., 2001). ABA-induced stomatal closure is driven by an efflux of K+ from guard cells; the ions pass through voltage-dependent outward-rectifying K+ channels in the plasma membrane. Activation of K+ channels requires depolarization of the membrane, achieved principally by activating anion channels within the membrane (Schroeder et al., 1987; Negi et al., 2008; Vahisalu et al., 2008; Kim et al., 2010). ABA-dependent depolarization of the membrane has been suggested to be achieved in part by the inhibition of plasma membrane H+-ATPase action (Shimazaki et al., 1986; Goh et al., 1996; Roelfsema et al., 1998). In support of this contention, an ost2 missense mutant that constitutively expresses a highly active form of H+-ATPase AHA1 did not exhibit ABA-induced stomatal closure (Merlot et al., 2007). Inhibition of H+-ATPase by ABA is attributable to reduced phosphorylation of the penultimate Thr of the enzyme (Zhang et al., 2004; Hayashi et al., 2011). More recently, three basic helix-loop-helix (bHLH) transcription factors termed AKSs (ABA-responsive kinase substrates) have been shown to become phosphorylated in response to ABA (Takahashi et al., 2013). Proteins in the AKS family facilitate stomatal opening by increasing transcription of genes encoding inward-rectifying K+ channels, and ABA suppresses the activities of these channels by triggering the phosphorylation of transcription factors in the AKS family.

Several ABA receptors have been described. These include the Mg-chelatase H subunit (CHLH) (Shen et al., 2006; Wu et al., 2009; Du et al., 2012), G-protein-coupled receptor 2 (GCR2) (Liu et al., 2007), and the G-protein-coupled receptor-type G proteins GTG1 and GTG2 (Pandey et al., 2009). However, the suggestion that CHLH and GCR2 act as ABA receptors remains controversial (McCourt and Creelman, 2008; Cutler et al., 2010). Apart from these candidates, a family of START domain proteins, termed the PYR/PYL/RCARs (pyrabactin resistace/pyrabactin resistance 1-like/regulatory component of ABA receptor) has recently been convincingly identified as cytosolic ABA receptors, and recognition of ABA by these proteins activates members of the protein kinase SRK2/SnRK2 family, including OST1, via inactivation of centrally acting negative regulators, the type 2C protein phosphatases (PP2Cs) that include ABI1 and ABI2 (Ma et al., 2009; Park et al., 2009; Kim et al., 2010; Nishimura et al., 2010). Today, an early acting ABA-signaling pathway, PYR/PYL/RCARs-PP2Cs-SRK2/SnRK2s, is considered to mediate most ABA-triggered plant responses, including the inhibition of seed germination and root growth, stomatal closure, and the expression of particular genes (Cutler et al., 2010). Notably, ABA-dependent phosphorylation of the bHLH transcription factors (the AKSs in guard cells) is also mediated by the PYR/PYL/RCARs-PP2Cs-SRK2/SnRK2s pathway (Takahashi et al., 2013).

The CHLH of chloroplasts was reported to serve as an ABA receptor, mediating ABA-dependent inhibition of seed germination and root growth, ABA-induced expression of certain genes, and ABA-dependent stomatal closure (Shen et al., 2006; Wu et al., 2009; Du et al., 2012). CHLH is a multifunctional protein involved in chlorophyll synthesis (Gibson et al., 1995; Willows et al., 1996; Huang and Li, 2009), retrograde plastid-to-nucleus signaling (Mochizuki et al., 2001), and ABA signaling. Recently, a rapid transpiration in detached leaves 1 (rtl1) mutant bearing a novel missense mutation in the H subunit of Mg-chelatase (CHLH) was isolated from ethyl methanesulfonate (EMS)-treated Arabidopsis thaliana using screen seeking mutants altered in terms of stomatal aperture (Tsuzuki et al., 2011). Stomatal movements in the rtl1 mutant were insensitive to ABA, but ABA continued to normally influence seed germination and root growth. Moreover, the recombinant CHLH protein did not bind to [3H]-labeled ABA. Therefore, the question of whether CHLH indeed functions as an ABA receptor, and mediates ABA-dependent inhibition of seed germination and root growth (Müller and Hansson, 2009; Tsuzuki et al., 2011), remains controversial. Moreover, the rtl1 mutant exhibited ABA-induced stomatal closure in the presence of a high concentration of extracellular Ca2+, suggesting that CHLH affects Ca2+ signaling in guard cells (Tsuzuki et al., 2011). However, the molecular mechanism by which CHLH mediates ABA-signaling in such cells remains largely unknown.

In the present study, we further analyzed CHLH function in guard cells and tried to manipulate stomatal aperture using CHLH. First, we examined ABA-dependent gene expression and phosphorylation of AKSs in guard cell protoplasts (GCPs) from the rtl1 mutant and concluded that CHLH did not affect these processes. Furthermore, we found that CHLH reduced the ABA mediated de-phosphorylation of guard-cell H+-ATPase. Finally, we obtained direct evidence that overexpression of CHLH in guard cells confers drought tolerance on Arabidopsis plants by increasing the sensitivity of stomatal guard cells to ABA.

Materials and methods

Plant materials and growth conditions

Plants of A. thaliana ecotype Columbia gl1 (glabrous1) served as wild-type (WT) plants. The background ecotype of the rtl1 mutation is gl1 (Tsuzuki et al., 2011), Ler (Landsberg erecta) is the background ecotype of abi1-1 (Leung et al., 1997), and Col is the background ecotype of a cch mutant (Mochizuki et al., 2001). The abi1-1 mutant was obtained from the Arabidopsis Biological Resource Center (Ohio State University, Columbus, OH, USA). Plants were grown in soil under a 16-h fluorescent light (50 μmol m−2 s−1)/8-h dark cycle at 24°C at a relative humidity of 55–75% for 4–6 weeks in a dedicated growth room (Kinoshita et al., 2001).

Isolation of GCPs and ABA treatment

GCPs from 5-week-old rosette leaves (~10 g) were enzymatically prepared as described by Ueno et al. (2005). To analyze ABA-responsive gene expression, GCPs were incubated in buffer (5 mM MES-NaOH, 10 mM KCl, 0.4 M mannitol, 1 mM CaCl2) supplemented (or not) with 20 μM ABA in the dark for 1 h at 24°C. For protein blot analysis and detection of 14-3-3 protein, GCPs were incubated in the above buffer with or without 20 μM ABA in the dark for 10 min at 24°C.

Quantification of mRNAs transcribed from ABA-responsive genes

Real-time quantitative polymerase chain reaction (PCR) was performed as described by Kinoshita et al. (2011) using the Power SYBR Green PCR Master Mix and the Step One Real-Time PCR system (Applied Biosystems, Foster City, CA, USA). Total RNA was isolated from GCPs using RNeasy Plant Mini Kits (Qiagen, Valencia, CA, USA), and first-strand cDNA was synthesized using Takara PrimeScript II 1st Strand cDNA Synthesis Kits (Takara, Tokyo, Japan). To specifically amplify RAB18 (At5g66400) and RD29B (At5g52300) transcripts, the following primer sets were used: for RAB18, 5′-TGTAACGCAGTCGCATTCG-3′ and 5′-CACATCGCAGGACGTACATACAT-3′; and for RD29B, 5′-CGAGCAAGACCCAGAAGTTCAC-3′ and 5′-TTACCCGTTACACCACCTCTCA-3′. Relative quantification of target gene expression levels was achieved using the comparative Ct (threshold cycle) method, and expression levels were normalized to that of TUB2 (At5g62690) transcripts (internal control) amplified using the primer pair 5′-AAACTCACTACCCCCAGCTTTG-3′ and 5′-CACCAGACATAGTAGCAGAAATCAAGT-3′. Three replicates were prepared in each experiment and the assays were repeated three times.

Immunoblot and protein blot analysis

Immunoblotting for 14-3-3 protein and protein blot analysis of GCPs were conducted as described by Takahashi et al. (2013). Thirty microgram amounts of guard cell proteins were separated by sodium dodecyl sulfate-polyacrylamide gel electrophoresis and transferred to nitrocellulose membranes. Twenty-five microgram amounts of protein from epidermal fragments were used when immunoblotting for CHLH. Epidermal fragments, including guard cells, were obtained as described by Hayashi et al. (2011), with some modifications. Fully expanded rosette leaves were harvested from each experimental dark-adapted 4–6 week-old plant and blended for 7 s in 35 ml of Milli-Q water (Millipore, Billerica, MA, USA) using a Waring blender equipped with an MC1 mini container (Waring Commercial, Odessa, FL, USA). Epidermal fragments were collected by retention on nylon mesh (58 μm in pore diameter), rinsed in Milli-Q water, and stored in a basal buffer containing 5 mM MES-BTP (pH 6.5), 50 mM KCl, and 0.1 mM CaCl2. The 14-3-3 proteins and CHLH were detected using an anti-14-3-3 protein (GF14ø) antibody and an anti-CHLH antibody, respectively (Kinoshita and Shimazaki, 1999; Tsuzuki et al., 2011); both antibodies were used at 3000-fold dilutions. An anti-goat IgG antibody conjugated with horseradish peroxidase (HRP) (Bio-Rad Laboratories, Hercules, CA, USA) was used at a dilution of 1:3,000 as a secondary antibody, and incubation proceeded at room temperature for 2 h. Chemiluminescence developing upon reaction of HRP with a substrate (Pierce, Rockford, IL, USA) was detected using the Light Capture AE-2150 system (Atto, Tokyo, Japan). For protein blot analysis, each nitrocellulose membrane was incubated with 0.1 μM GST-14-3-3 for 16 h at 4°C, and next with an anti-GST antibody (GE Healthcare UK Ltd., Buckinghamshire, UK) at a dilution of 1:3000 for 2 h at room temperature. The membrane was then exposed to an anti-goat IgG secondary antibody conjugated with HRP at a dilution of 1:3000 for 2 h at room temperature and the HRP-substrate reaction detected as described above.

Immunohistochemical detection of plasma membrane H+-ATPase in guard cells

Epidermal fragments were incubated for 20 min under background red light (RL; LED-R, Eyela, Tokyo, Japan) at 50 μmol m−2 s−1. BL (Stick-B-32, Eyela) at 10 μmol m−2 s−1 was applied to RL-illuminated epidermal fragments, thus being superimposed on the background RL, for 2.5 min. The phosphorylation status of epidermal guard cell H+-ATPase was immunohistochemically evaluated using the method of Hayashi et al. (2011). Epidermal fragments were incubated with anti-H+-ATPase and anti-pThr antibodies, which specifically recognize the catalytic domain and the phosphorylated threonine, respectively, of H+-ATPase (Hayashi et al., 2010). Both antibodies were added at a dilution of 1:1000 (w/v) in phosphate-buffered saline (PBS; 137 mM NaCl, 8.1 mM Na2HPO4, 2.68 mM KCl, 1.47 mM KH2PO4) with 3% (w/v) bovine serum albumin Fraction V (BSA; Sigma, St. Louis, MO, USA) and incubation proceeded at 37°C overnight. All samples were washed six times for 5 min each time with PBS and incubated with Alexa Fluor 488 goat anti-rabbit IgG (Invitrogen, Carlsbad, CA, USA) at a dilution of 1:500 in PBS with 3% (w/v) BSA at 37°C for 3 h in the dark. After washing a further six times for 5 min each time with PBS, each specimen was mounted on a glass slide using 50% (v/v) glycerol. Specimens were observed under a fluorescence microscope (BX50; Olympus, Tokyo, Japan) using the narrow excitation band-pass filter set BP460–480HQ BA495–540HQ (U-MGFPHQ; Olympus) to detect signal from Alexa Fluor 488. A Hg arc lamp was used as a source of excitation. Fluorescent images were collected using a CCD camera (DP72; Olympus) and processed with the aid of DP2-BSW software (Olympus). To estimate fluorescence intensities, all exposure times were identical (334.79 ms). The fluorescence intensities of stomata (>30 stomata/treatment) were determined via a zone densitometry method using CS Analyzer version 3.0 (Atto).

Measurement of stomatal aperture

Stomatal apertures were measured as described by Inoue et al. (2008). The stomatal aperture in the abaxial epidermal tissues of rosette leaves was measured microscopically. Stomatal apertures were the mean of 25 stomata and are shown with standard deviations (SDs). The data were confirmed by blind reassessment.

Drought tolerance test

Plants were grown in soil for 3 weeks under normal condition and then subjected to drought stress by withholding water for 18 days (Iuchi et al., 2001).

Vector construction and transformation

CHLH full-length cDNA was amplified by PCR with insertion of SalI sites upstream of the start codon and downstream of the stop codon using the primer pair 5′-ACGCGTCGACAAAATGGCTTCGCTTGTGTATTCTCC-3′ and 5′-ACGCGT CGACTCGATCGATCCCTTCGATCTTG-3′. The resulting PCR product was digested with SalI and subcloned into plasmid pUC18-CaMV35S::GFP (S65T) in a manner causing the 3′-end of the CHLH coding sequence to be fused in-frame to the 5′-end of GFP. CHLH-GFP was amplified by PCR with insertion of XbaI sites upstream of the CHLH start codon and downstream of the GFP stop codon using the primer pair 5′-GCCTCTAGAAAAATGGCTTCGCTTGTGTATTCTCCAT-3′ and 5′-GCCTCTAGATTACTTGTACAGCTCGTCCATGC-3′. The PCR product was ligated into the vector pPZP211-CER6 previously constructed by our group (Kinoshita et al., 2011). The resulting plasmid was introduced into Agrobacterium tumefaciens (GV3101), which was next transferred to plants using the floral dip method (Clough and Bent, 1998). Transgenic plants were selected on Murashige–Skoog agar plates containing the relevant antibiotic. F4 homozygous plants were used in all experiments.

Results

ABA induces expression of ABA-responsive genes in both the rtl1 mutant and WT plants

A recent study using a novel chlh mutant, rtl1, indicated that CHLH affects ABA-induced stomatal closure, but does not serve as an ABA receptor in A. thaliana, and that CHLH also does not affect other ABA-mediated phenomena, including seed germination and post-germination growth (Tsuzuki et al., 2011). However, whether CHLH affects ABA-induced expression of particular genes and/or ABA-induced phosphorylation of the bHLH transcription factors, the AKSs (Takahashi et al., 2013), in guard cells remains unclear. First, we performed quantitative PCR to determine the expression levels of typical ABA-responsive genes, RAB18 and RD29B (Leonhardt et al., 2004; Fujii et al., 2007), in GCPs. Incubation of WT GCPs with 20 μM ABA for 1 h induced expression of RAB18 and RD29B. Similarly, the expression levels of these genes increased in GCPs from the rtl1 mutant in response to ABA (Figure 1A). In contrast, GCPs from the abi1-1 mutant, which is an ABA-insensitive mutant with a lesion in the PYR/PYL/RCARs-PP2Cs-SRK2/SnRK2s pathway (Ma et al., 2009; Park et al., 2009; Nishimura et al., 2010), did not show ABA-induced gene expression (Figure 1B). These results indicated that CHLH did not affect the expression of ABA-responsive genes. Notably, the extent of induction of ABA-responsive genes in the rlt1 mutant was greater than seen in the WT. In accord with this, another CHLH missense mutant, cch (P642 to L), which shows ABA-insensitive phenotype in stomatal closure (Tsuzuki et al., 2011), also showed higher magnitude of induction of ABA-responsive genes in GCPs (Supplementary Figure S1). Further investigation will be needed to clarify greater induction of ABA-responsive genes in these mutants.

Figure 1.

Figure 1

Open in a new tab

ABA-responsive gene expression and ABA-induced phosphorylation of bHLH transcription factors (the AKSs) in guard cells from the rtl1 mutant. (A) The expression levels of ABA-responsive genes, RAB18 and RD29B, in GCPs from WT and rtl1 mutant plants, measured using real-time quantitative PCR. Transcript levels were normalized to that of TUB2. GCPs were incubated in the presence or absence of 20 μM ABA for 1 h. Data represent the means of three measurements ± standard deviations (SDs). (B) Expression of ABA-responsive genes in GCPs from abi1-1 and Ler plants. The experimental conditions were as described in (A) above. (C) ABA-induced protein phosphorylation in GCPs from WT and rtl1 plants. Phosphorylation of 43- and 53-kDa proteins was detected via protein blot analysis using GST-fused 14-3-3 protein as a probe (“Protein blot”), and endogenous 14-3-3 proteins were detected by immunoblotting using an anti-14-3-3 protein antibody (“Anti-14-3-3 protein”). GCPs were incubated in the presence or absence of 20 μM ABA for 10 min. The lower panel shows the relative phosphorylation levels of the AKSs, and the 43- and 53-kDa proteins, quantified by calculating the ratios of the signal intensities of the protein blot bands to those of immunoblot bands of 14-3-3 proteins. The data are expressed relative to the level of phosphorylation in ABA-untreated WT plants. The experiment was repeated twice on different occasions and yielded similar results.

Next, we performed protein blot analysis using 14-3-3 protein as a probe to examine ABA-induced phosphorylation of AKSs in GCPs because the 14-3-3 protein specifically binds to phosphorylated AKSs (Takahashi et al., 2013). As shown in Figure 1C, ABA-induced phosphorylation of AKSs (53 and 43 kDa in size) was evident in both WT and rtl1 GCPs. These results indicated that CHLH had no effect on ABA-induced phosphorylation of AKSs.

CHLH affects ABA-induced inhibition of BL-induced phosphorylation of guard cell H+-ATPase

Previous work indicated that ABA inhibits BL-mediated stomatal opening at least in part via induction of the dephosphorylation of guard cell H+-ATPase (Zhang et al., 2004; Hayashi and Kinoshita, 2011; Hayashi et al., 2011). Thus, we used an immunohistochemical method to investigate the phosphorylation status of guard cell H+-ATPase in the epidermis. In WT plants, guard cell H+-ATPase was dephosphorylated under exposure to RL, and BL superimposed on RL induced phosphorylation of the H+-ATPase. Furthermore, preincubation of the epidermis with 20 μM ABA completely suppressed this BL-induced phosphorylation. Moreover, inhibition of BL-induced phosphorylation of the H+-ATPase by ABA was severely suppressed in the rtl1 mutant (Figures 2A,B). In addition, the mutant exhibited relatively higher phosphorylation levels of guard cell H+-ATPase (compared to the WT) both before and after BL illumination. The observed changes in the phosphorylation level of H+-ATPase were not attributable to differences in the amounts of H+-ATPase between strains; the treatment used had no effect on the levels of guard cell H+-ATPase in WT or rtl1 plants. These results suggest that CHLH mediates not only the induction of ABA-induced stomatal closure but also the ABA inhibition of BL-induced phosphorylation of guard cell H+-ATPase.

Figure 2.

Figure 2

Open in a new tab

Effect of ABA on blue light (BL)-induced H+-ATPase phosphorylation in stomatal guard cells of the rtl1 mutant. Epidermal fragments of rosette leaves from WT and rtl1 mutant plants were illuminated with red light (RL) for 20 min and then illuminated by BL superimposed on the background RL (RL+BL) for 2.5 min. ABA (20 μM) was added to epidermal fragments 20 min before BL illumination commenced (RL+BL+ABA). (A) Typical images of stomata immunostained using anti-pThr and anti-H+-ATPase antibodies. Scale bar = 10 μm. (B) Fluorescent signal intensities from stomata immunostained with anti-pThr antibody. Values represent the mean ± SD (n = 30) in arbitrary units (a.u.). The experiment was repeated three times on different occasions with similar results.

CHLH transgenic plants exhibit closed-stomata and drought tolerance phenotypes

Knockdown of CHLH is reportedly associated with open-stomata and ABA-insensitive phenotypes of stomatal guard cells (Shen et al., 2006; Legnaioli et al., 2009; Tsuzuki et al., 2011), suggesting that overexpression of CHLH in guard cells may induce stomatal closure and increase sensitivity to ABA. We therefore constructed CHLH-GFP transgenic plants using the CER6 promoter to drive overexpression of CHLH-GFP in epidermal tissue including guard cells (Hooker et al., 2002; Kinoshita et al., 2011). As shown in Figure 3A, GFP-derived fluorescence was observed in guard cells from CHLH-GFP transgenic plants. Immunoblotting of epidermal fragments revealed that CHLH-GFP was specifically detected in CHLH-GFP transgenic plants, in addition to endogenous CHLH (Figure 3B). Note that the epidermal fragments used in immunoblotting analysis contained not only epidermal and guard cells but also mesophyll cells attached to the epidermis (Supplementary Figure S2). Therefore, the signal from endogenous CHLH likely emanated from mesophyll cells in addition to epidermal tissue. According to the available expression database, Arabidopsis eFP Browser, expression level of CER6, which is used for expression of CHLH-GFP, is higher than that of the endogenous CHLH in guard cells. Thus, amount of CHLH-GFP may be higher than endogenous CHLH in guard cells. In contrast, CHLH-GFP was expressed only in epidermal tissue because CHLH-GFP expression was driven by the epidermis-specific CER6 promoter. The signal intensity of GFP from CHLH-GFP showed that the recombinant protein was expressed principally in guard cells of the epidermis (Figure 3A).

Figure 3.

Figure 3

Open in a new tab

Phenotypic analysis of CHLH transgenic plants. The phenotypes of two independent CER6::CHLH-GFP plants were compared with that of WT plants. (A) Typical bright-field and GFP fluorescent images of stomata in the abaxial epidermis of rosette leaves. Scale bar = 10 μm. (B) Immunoblots using anti-CHLH antibody showing CHLH-GFP and endogenous CHLH in GCPs. (C) The stomatal aperture in 4-week-old plants exposed to light conditions at zeitgeber time (ZT) 4. Epidermal fragments were isolated from rosette leaves and apertures measured immediately. Data represent the means of 25 measurements ±SDs. Pairs for Student's t-test are indicated with brackets (*P < 0.01). (D) Kinetics of fresh weight changes in detached rosette leaves from 4-week-old WT plants (open circles) and CER6::CHLH-GFP #1 (closed circles) and #2 (closed squares). The relative weights of leaves are presented (±SD) as percentages of initial weights, being the weights of rosette leaves immediately after detachment from plants (n = 6). (E) Drought tolerance in WT and CHLH-GFP transgenic plants. Plants grown in soil for 3 weeks were subjected to drought stress by withholding water for 18 days. (F) Effect of ABA on the stomatal aperture of WT and CHLH-GFP transgenic plants. Epidermal fragments isolated from rosette leaves of 4-week-old plants exposed to light at ZT 4 were treated with ABA at the indicated concentrations for 2.5 h under BL superimposed on background red light. The stomatal apertures in the abaxial epidermis were measured microscopically. Data represent the means of 25 measurements ±SDs. Asterisks indicate significant differences between wild type and each CHLH-transgenic plants under 0 μM ABA (*P < 0.05; Student's t-test). The experiment was repeated three times on different occasions with similar results.

We next measured stomatal aperture under conditions of light exposure. The stomata of CHLH-GFP transgenic plants were notably more closed than those of WT plants (Figure 3C). Moreover, leaves detached from CHLH-GFP transgenic plants lost weight only slowly under light-exposure conditions (Figure 3D). The average weight of rosette leaves detached from WT plants fell to about 70% of their initial weight over 90 min, whereas the weights of leaves from CHLH-GFP transgenic plants decreased to about 80% of their initial weight. These results indicate that CHLH-GFP transgenic plants express the closed-stomata phenotype even under conditions of light exposure.

Next, we examined drought tolerance in CHLH-GFP transgenic plants. Plants were grown for 3 weeks under normal conditions and next exposed to drought stress by withholding water for 18 days. Most WT plants died, while all CHLH-GFP transgenic plants survived. To assess whether the enhanced drought tolerance of CHLH-GFP transgenic plants was attributable to an alteration in sensitivity to ABA, we measured the effect of ABA on the stomatal aperture (Figure 3F). The results showed that the stomata of CHLH-GFP transgenic, but not WT, plants closed in response to a low concentration (1 μM) of ABA, although a high level of ABA (20 μM) induced stomatal closure in both types of plants. It should be noted that the differences of stomatal aperture between wild type and CHLH-transgenic plants in Figure 3F (0 μM ABA) were smaller than that in Figure 3C, since the epidermal tissues were incubated with a buffer containing 50 mM K+, which facilitates stomatal opening, for 2.5 h under light in Figure 3F. However, the differences were significant. Together, the results indicate that overexpression of CHLH in guard cells confers drought tolerance via promotion of stomatal closure and that this is probably attributable to enhanced sensitivity of guard cells to ABA.

Discussion

CHLH specifically affects ABA-dependent stomatal closure but not ABA-induced gene expression in guard cells

A previous study using a novel chlh mutant, rtl1, indicated that CHLH specifically affected ABA-induced stomatal closure (Supplementary Figure S3) but not germination or post-germination growth (Tsuzuki et al., 2011). In the present study, we have provided evidence that CHLH has no effect on the expression of ABA-responsive genes, such as RAB18 and RD29B, in guard cells. A study suggested that the expression of ABA-responsive genes is mediated by an early ABA-signaling pathway, PYR/PYL/RCARs-PP2Cs-SRK2/SnRK2s (Saavedra et al., 2010). Together, the results suggest that CHLH specifically affects ABA-dependent stomatal closure but not regulation of ABA-responsive genes in guard cells via the PYR/PYL/RCARs-PP2Cs-SRK2/SnRK2s pathway (Figure 1A). Recently, three bHLH transcription factors, the AKSs, which control the expression of inward-rectifying K+ channels of the plasma membrane (including KAT1 and AKT2), have been shown to become phosphorylated in guard cells in response to ABA, and such phosphorylation is most likely mediated by the PYR/PYL/RCARs-PP2Cs-SRK2/SnRK2s pathway (Takahashi et al., 2013). However, GCPs of the rtl1 mutant exhibited normal ABA-dependent phosphorylation of AKSs (Figure 1C). The results thus also suggest that CHLH has no effect on PYR/PYL/RCARs-PP2Cs-SRK2/SnRK2s pathway-mediated ABA-dependent phosphorylation of AKSs in guard cells.

CHLH affects the phosphorylation status of guard-cell H+-ATPase

We recently established an immunohistochemical method for detecting BL-induced and phototropin-mediated phosphorylation of plasma membrane H+-ATPase in the stomatal guard cells of A. thaliana (Hayashi et al., 2011). The technique allows one to measure the phosphorylation/activation status of guard cell H+-ATPase in the epidermis of a single rosette leaf, and thus eliminates the need to prepare GCPs from a large number of plants. Moreover, the method can be used to detect guard cell responses under more natural and stress-free conditions. Protoplast preparation stresses plants. We took advantage of these properties to examine the effect of ABA on BL-induced phosphorylation of guard cell H+-ATPase using ABA-insensitive mutants, including abi1-1, abi2-1, and ost1-2. The results indicated that an early ABA signaling pathway, the PYR/PYL/RCAR-PP2Cs-SRK2/SnRK2s pathway (Ma et al., 2009; Park et al., 2009; Nishimura et al., 2010), was involved in ABA-induced inhibition of BL-induced phosphorylation of guard cell H+-ATPase (Hayashi and Kinoshita, 2011; Hayashi et al., 2011). In the present study, we used an immunohistochemical method to examine the phosphorylation status of the guard cell H+-ATPase of the rtl1 mutant and found that ABA-induced inhibition of BL-induced H+-ATPase phosphorylation was greatly suppressed in the rtl1 mutant (Figures 2A,B). In addition, the rtl1 mutant exhibited a higher level of phosphorylation of guard cell H+-ATPase prior to BL illumination than the WT. These results suggest that CHLH affects ABA-induced inhibition of the BL-induced phosphorylation of the penultimate Thr of guard cell H+-ATPase, and that this inhibition is mediated by both the PYR/PYL/RCARs-PP2Cs-SRK2/SnRK2s pathway and CHLH. Further investigation is needed to clarify the relationship between the PYR/PYL/RCARs-PP2Cs-SRK2/SnRK2s pathway and CHLH in this context.

CHLH overexpression confers drought tolerance via promotion of stomatal closure

In the present study, we found evidence that CHLH-GFP transgenic plants in which the CER6 promoter drives the CHLH-GFP exhibited a closed-stomata phenotype under light conditions (Figures 3C,D), and drought tolerance, probably via increased sensitivity to ABA (Figures 3E,F). Previously, CHLH overexpression driven by the CaMV35S promoter, which induces overexpression of CHLH in whole plant, was found to cause development of an ABA-hypersensitive phenotype in terms of stomatal movement and increased resistance to dehydration (Shen et al., 2006). However, previous study has not shown that CHLH overexpression causes drought tolerance. In addition, it is worthy of note that expression of Vicia faba VfPIP, a putative aquaporin gene, driven by the CaMV35S promoter in A. thaliana has been shown to improve their drought tolerance at least in part through lower transpiration phenotype, although the VfPIP transgenic plants had longer primary and lateral roots, and a greater number of lateral roots than the control plants (Cui et al., 2008). To our knowledge, the present result is the first report to demonstrate that overexpression of CHLH in guard cells confers drought tolerance via manipulation of the stomatal aperture. Our results suggest that manipulation of the stomatal aperture via overexpression of CHLH in guard cells may prove very useful to improve drought tolerance in plants of economic importance.

Conflict of interest statement

The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.

Acknowledgments

We thank M. Goto, M. Hayashi, and Y. Hayashi for providing excellent technical assistance. This work was supported in part by Grants-in-Aid for Scientific Research (nos. 22119005 and 21227001) from the Ministry of Education, Culture, Sports, Science and Technology, Japan (Toshinori Kinoshita), and by an ALCA grant from the Japan Science and Technology Agency (Toshinori Kinoshita).

Supplementary material

The Supplementary Material for this article can be found online at: http://www.frontiersin.org/journal/10.3389/fpls.2013.00440/abstract

Supplementary Figure S1

ABA-responsive gene expression in guard cells from cch. Expression level of ABA-responsible genes, RAB18 and RD29B in GCPs from cch and wild-type (Col-0) plants determined by real-time quantitative PCR. Transcript abundance of each gene was normalized to TUB2. GCPs were incubated in the presence or absence of 20 μM ABA for 1 h. Data represent means of three technical measurements with the standard deviation (SD).

Click here for additional data file. (2.1MB, ZIP)
Supplementary Figure S2

Typical epidermal fragments used in the present study. Epidermal fragments were obtained by blending rosette leaves and subsequent collection of material on 58-μm-pore-sized nylon mesh as described in the Materials and Methods. Scale bar = 50 μm.

Click here for additional data file. (2.1MB, ZIP)
Supplementary Figure S3

Effect of ABA on stomatal aperture of the rtl1 mutant. Epidermal fragments isolated from dark-adapted rtl1 and WT plants were illuminated with BL superimposed on the background RL (RL+BL) for 2.5 h. ABA (20 μM) was added to epidermal fragments 20 min before BL illumination commenced (RL+BL+ABA). As a control, the epidermal fragments were incubated in the dark for 2.5 h (Dk). The stomatal apertures in the abaxial epidermis was measured microscopically. The data represent the means of 25 measurements ± SDs. The experiment was repeated three times on different occasions with similar results.

Click here for additional data file. (2.1MB, ZIP)

References

  1. Assmann S. M., Simoncini L., Schroeder J. I. (1985). Blue light activates electrogenic ion pumping in guard cell protoplasts of Vicia faba. Nature 318, 285–287 10.1038/318285a0 [DOI] [Google Scholar]
  2. Clough S. J., Bent A. F. (1998). Floral dip: a simplified method for Agrobacterium-mediated transformation of Arabidopsis thaliana. Plant J. 16, 735–743 10.1046/j.1365-313x.1998.00343.x [DOI] [PubMed] [Google Scholar]
  3. Cui X. H., Hao F. S., Chen H., Chen J., Wang X. C. (2008). Expression of the Vicia faba VfPIP1 gene in Arabidopsis thaliana plants improves their drought resistance. J. Plant Res. 121, 207–214 10.1007/s10265-007-0130-z [DOI] [PubMed] [Google Scholar]
  4. Cutler S. R., Rodriguez P. L., Finkelstein R. R., Abrams S. R. (2010). Abscisic acid: emergence of a core signaling network. Annu. Rev. Plant Biol. 61, 651–679 10.1146/annurev-arplant-042809-112122 [DOI] [PubMed] [Google Scholar]
  5. Du S. Y., Zhang X. F., Lu Z., Xin Q., Wu Z., Jiang T., et al. (2012). Roles of the different components of magnesium chelatase in abscisic acid signal transduction. Plant Mol. Biol. 80, 519–537 10.1007/s11103-012-9965-3 [DOI] [PMC free article] [PubMed] [Google Scholar]
  6. Fujii H., Verslues P. E., Zhu J. K. (2007). Identification of two protein kinases required for abscisic acid regulation of seed germination, root growth, and gene expression in Arabidopsis. Plant Cell. 19, 485–494 10.1105/tpc.106.048538 [DOI] [PMC free article] [PubMed] [Google Scholar]
  7. Gibson L. C. D., Willows R. D., Kannangara C. G., von Wettstein D., Hunter C. N. (1995). Magnesium-protoporphyrin chelatase of Rhodobacter sphaeroides: reconstitution of activity by combining the products of the bchH, -I and -D genes expressed in Escherichia coli. Proc. Natl. Acad. Sci. U.S.A. 92, 1941–1944 10.1073/pnas.92.6.1941 [DOI] [PMC free article] [PubMed] [Google Scholar]
  8. Goh C. H., Kinoshita T., Oku T., Shimazaki K. (1996). Inhibition of blue light-dependent H+ pumping by abscisic acid in Vicia guard-cell protoplasts. Plant Physiol. 111, 433–440 [DOI] [PMC free article] [PubMed] [Google Scholar]
  9. Hayashi M., Inoue S., Takahashi K., Kinoshita T. (2011). Immunohistochemical detection of blue light-induced phosphorylation of the plasma membrane H+-ATPase in stomatal guard cells. Plant Cell Physiol. 52, 1238–1248 10.1093/pcp/pcr072 [DOI] [PubMed] [Google Scholar]
  10. Hayashi M., Kinoshita T. (2011). Crosstalk between blue-light- and ABA-signaling pathways in stomatal guard cells. Plant Sig. Behav. 6, 1662–1664 10.4161/psb.6.11.17800 [DOI] [PMC free article] [PubMed] [Google Scholar]
  11. Hayashi Y., Nakamura S., Takemiya A., Takahashi Y., Shimazaki K., Kinoshita T. (2010). Biochemical characterization of in vitro phosphorylation and dephosphorylation of the plasma membrane H+-ATPase. Plant Cell Physiol. 51, 1186–1196 10.1093/pcp/pcq078 [DOI] [PubMed] [Google Scholar]
  12. Hooker T. S., Millar A. A., Kunst L. (2002). Significance of the expression of the CER6 condensing enzyme for cuticular wax production in Arabidopsis. Plant Physiol. 129, 1568–1580 10.1104/pp.003707 [DOI] [PMC free article] [PubMed] [Google Scholar]
  13. Huang Y. S., Li H. (2009). Arabidopsis CHLI2 can substitute for CHLI1. Plant Physiol. 150, 636–645 10.1104/pp.109.135368 [DOI] [PMC free article] [PubMed] [Google Scholar]
  14. Inoue S., Kinoshita T., Matsumoto M., Nakayama K., Doi M., Shimazaki K. (2008). Blue light-induced autophosphorylation of phototropin is a primary step for signaling. Proc. Natl. Acad. Sci. U.S.A. 105, 5626–5631 10.1073/pnas.0709189105 [DOI] [PMC free article] [PubMed] [Google Scholar]
  15. Iuchi S., Kobayashi M., Taji T., Naramoto M., Seki M., Kato T., et al. (2001). Regulation of drought tolerance by gene manipulation of 9-cis-epoxycarotenoid dioxygenase, a key enzyme in abscisic acid biosynthesis in Arabidopsis. Plant J. 27, 325–333 10.1046/j.1365-313x.2001.01096.x [DOI] [PubMed] [Google Scholar]
  16. Kim T. H., Böhmer M., Hu H., Nishimura N., Schroeder J. I. (2010). Guard cell signal transduction network: advances in understanding abscisic acid, CO2, and Ca2+ signaling. Annu. Rev. Plant Biol. 61, 561–591 10.1146/annurev-arplant-042809-112226 [DOI] [PMC free article] [PubMed] [Google Scholar]
  17. Kinoshita T., Hayashi Y. (2011). New insights into the regulation of stomatal opening by blue light and the plasma membrane H+-ATPase. Int. Rev. Cell Mol. Biol. 289, 89–115 10.1016/B978-0-12-386039-2.00003-1 [DOI] [PubMed] [Google Scholar]
  18. Kinoshita T., Shimazaki K. (1999). Blue light activates the plasma membrane H+-ATPase by phosphorylation of the C-terminus in stomatal guard cells. EMBO J. 18, 5548–5558 10.1093/emboj/18.20.5548 [DOI] [PMC free article] [PubMed] [Google Scholar]
  19. Kinoshita T., Shimazaki K. (2002). Biochemical evidence for the requirement of 14-13-3 protein binding in activation of the guard-cell plasma membrane H+-ATPase by blue light. Plant Cell Physiol. 43, 1359–1365 10.1093/pcp/pcf167 [DOI] [PubMed] [Google Scholar]
  20. Kinoshita T., Doi M., Suetsugu N., Kagawa T., Wada M., Shimazaki K. (2001). phot1 and phot2 mediate blue light regulation of stomatal opening. Nature 414, 656–660 10.1038/414656a [DOI] [PubMed] [Google Scholar]
  21. Kinoshita T., Ono N., Hayashi Y., Morimoto S., Nakamura S., Soda M., et al. (2011). FLOWERING LOCUS T regulates stomatal opening. Curr. Biol. 21, 1232–1238 10.1016/j.cub.2011.06.025 [DOI] [PubMed] [Google Scholar]
  22. Legnaioli T., Cuevas J., Mas P. (2009). TOC1 functions as a molecular switch connecting the circadian clock with plant responses to drought. EMBO J. 28, 3745–3757 10.1038/emboj.2009.297 [DOI] [PMC free article] [PubMed] [Google Scholar]
  23. Leonhardt N., Kwak J. M., Robert N., Waner D., Leonhardt G., Schroeder J. I. (2004). Microarray expression analyses of Arabidopsis guard cells and isolation of a recessive abscisic acid hypersensitive protein phosphatase 2C mutant. Plant Cell. 16, 596–615 10.1105/tpc.019000 [DOI] [PMC free article] [PubMed] [Google Scholar]
  24. Leung J., Merlot S., Giraudat J. (1997). The Arabidopsis ABSCISIC ACID-INSENSITIVE2 (ABI2) and ABI1 genes encode homologous protein phosphatases 2C involved in abscisic acid signal transduction. Plant Cell. 9, 759–771 10.2307/3870430 [DOI] [PMC free article] [PubMed] [Google Scholar]
  25. Liu X., Yue Y., Li B., Nie Y., Li W., Wu W. H., et al. (2007). A G protein-coupled receptor is a plasma membrane receptor for the plant hormone abscisic acid. Science 315, 1712–1716 10.1126/science.1135882 [DOI] [PubMed] [Google Scholar]
  26. Ma Y., Szostkiewicz I., Korte A., Moes D., Yang Y., Christmann A., et al. (2009). Regulators of PP2C phosphatase activity function as abscisic acid sensors. Science 324, 1064–1068 10.1126/science.1172408 [DOI] [PubMed] [Google Scholar]
  27. McCourt P., Creelman R. (2008). The ABA receptors—we report you decide. Curr. Opin. Plant Biol. 11, 474–478 10.1016/j.pbi.2008.06.014 [DOI] [PubMed] [Google Scholar]
  28. Merlot S., Leonhardt N., Fenzi F., Valon C., Costa M., Piette L., et al. (2007). Constitutive activation of a plasma membrane H+-ATPase prevents abscisic acid-mediated stomatal closure. EMBO J. 26, 3216–3226 10.1038/sj.emboj.7601750 [DOI] [PMC free article] [PubMed] [Google Scholar]
  29. Mochizuki N., Brusslan J. A., Larkin R., Nagatani A., Chory J. (2001). Arabidopsis genomes uncoupled 5 (GUN5) mutant reveals the involvement of Mg-chelatase H subunit in plastid-to-nucleus signal transduction. Proc. Natl. Acad. Sci. U.S.A. 98, 2053–2058 10.1073/pnas.98.4.2053 [DOI] [PMC free article] [PubMed] [Google Scholar]
  30. Müller A. H., Hansson M. (2009). The barley magnesium chelatase 150-kD subunit is not an abscisic acid receptor. Plant Physiol. 150, 157–166 10.1104/pp.109.135277 [DOI] [PMC free article] [PubMed] [Google Scholar]
  31. Negi J., Matsuda O., Nagasawa T., Oba Y., Takahashi H., Kawai-Yamada M., et al. (2008). CO2 regulator SLAC1 and its homologues are essential for anion homeostasis in plant cells. Nature 452, 483–486 10.1038/nature06720 [DOI] [PubMed] [Google Scholar]
  32. Nishimura N., Sarkeshik A., Nito K., Park S. Y., Wang A., Carvalho P. C., et al. (2010). PYR/PYL/RCAR family members are major in-vivo ABI1 protein phosphatase 2C-interacting proteins in Arabidopsis. Plant J. 61, 290–299 10.1111/j.1365-313X.2009.04054.x [DOI] [PMC free article] [PubMed] [Google Scholar]
  33. Pandey S., Nelson D. C., Assmann S. M. (2009). Two novel GPCR-type G proteins are abscisic acid receptors in Arabidopsis. Cell 136, 136–148 10.1016/j.cell.2008.12.026 [DOI] [PubMed] [Google Scholar]
  34. Park S. Y., Fung P., Nishimura N., Jensen D. R., Fujii H., Zhao Y., et al. (2009). Abscisic acid inhibits type 2C protein phosphatases via the PYR/PYL family of START proteins. Science 324, 1068–1071 10.1126/science.1173041 [DOI] [PMC free article] [PubMed] [Google Scholar]
  35. Roelfsema M. R. G., Staal M., Prins H. B. A. (1998). Blue light-induced apoplastic acidification of Arabidopsis thaliana guard cells: inhibition by ABA is mediated through protein phosphatases. Physiol. Plant. 103, 466–474 10.1034/j.1399-3054.1998.1030404.x [DOI] [Google Scholar]
  36. Saavedra X., Modrego A., Rodríguez D., González-García M. P., Sanz L., Nicolás G., et al. (2010). The nuclear interactor PYL8/RCAR3 of Fagus sylvatica FsPP2C1 is a positive regulator of abscisic acid signaling in seeds and stress. Plant Physiol. 152, 133–150 10.1104/pp.109.146381 [DOI] [PMC free article] [PubMed] [Google Scholar]
  37. Schroeder J. I., Allen G. J., Hugouvieux V., Kwak J. M., Waner D. (2001). Guard cell signal transduction. Annu. Rev. Plant Physiol. Plant Mol. Biol. 52, 627–658 10.1146/annurev.arplant.52.1.627 [DOI] [PubMed] [Google Scholar]
  38. Schroeder J. I., Raschke K., Neher E. (1987). Voltage dependence of K channels in guard-cell protoplasts. Proc. Natl. Acad. Sci. U.S.A. 84, 4108–4112 10.1073/pnas.84.12.4108 [DOI] [PMC free article] [PubMed] [Google Scholar]
  39. Shen Y. Y., Wang X. F., Wu F. Q., Du S. Y., Cao Z., Shang Y., et al. (2006). The Mg-chelatase H subunit is an abscisic acid receptor. Nature 443, 823–826 10.1038/nature05176 [DOI] [PubMed] [Google Scholar]
  40. Shimazaki K., Doi M., Assmann S. M., Kinoshita T. (2007). Light regulation of stomatal movement. Annu. Rev. Plant Biol. 58, 219–247 10.1146/annurev.arplant.57.032905.105434 [DOI] [PubMed] [Google Scholar]
  41. Shimazaki K., Iino M., Zeiger E. (1986). Blue light-dependent proton extrusion by guard-cell protoplasts of Vicia faba. Nature 319, 324–326 10.1038/319324a016665408 [DOI] [Google Scholar]
  42. Takahashi Y., Ebisu Y., Kinoshita T., Doi M., Okuma E., Murata Y., et al. (2013). bHLH transcription factors that facilitate K+ uptake during stomatal opening are repressed by abscisic acid through phosphorylation. Sci. Signal. 6, 1–10 10.1126/scisignal.2003760 [DOI] [PubMed] [Google Scholar]
  43. Tsuzuki T., Takahashi K., Inoue S., Okigaki Y., Tomiyama M., Hossain M. A., et al. (2011). Mg-chelatase H subunit affects ABA signaling in stomatal guard cells, but is not an ABA receptor in Arabidopsis thaliana. J. Plant Res. 124, 527–538 10.1007/s10265-011-0426-x [DOI] [PMC free article] [PubMed] [Google Scholar]
  44. Ueno K., Kinoshita T., Inoue S., Emi T., Shimazaki K. (2005). Biochemical characterization of plasma membrane H+-ATPase activation in guard cell protoplasts of Arabidopsis thaliana in response to blue light. Plant Cell Physiol. 46, 955–963 10.1093/pcp/pci104 [DOI] [PubMed] [Google Scholar]
  45. Vahisalu T., Kollist H., Wang Y. F., Nishimura N., Chan W. Y., Valerio G., et al. (2008). SLAC1 is required for plant guard cell S-type anion channel function in stomatal signalling. Nature 452, 487–491 10.1038/nature06608 [DOI] [PMC free article] [PubMed] [Google Scholar]
  46. Willows R. D., Gibson L. C., Kanangara C. G., Hunter C. N., von Wettstein D. (1996). Three separate proteins constitute the magnesium chelatase of Rhodobacter sphaeroides. Eur. J. Biochem. 235, 438–443 10.1111/j.1432-1033.1996.00438.x [DOI] [PubMed] [Google Scholar]
  47. Wu F. Q., Xin Q., Cao Z., Liu Z. Q., Du S. Y., Mei C., et al. (2009). The magnesium-chelatase H subunit binds abscisic acid and functions in abscisic acid signaling: new evidence in Arabidopsis. Plant Physiol. 150, 1940–1954 10.1104/pp.109.140731 [DOI] [PMC free article] [PubMed] [Google Scholar]
  48. Zhang X., Wang H., Takemiya A., Song C. P., Kinoshita T., Shimazaki K. (2004). Inhibition of blue light-dependent H+ pumping by abscisic acid through hydrogen peroxide-induced dephosphorylation of the plasma membrane H+-ATPase in guard cell protoplasts. Plant Physiol. 136, 4150–4158 10.1104/pp.104.046573 [DOI] [PMC free article] [PubMed] [Google Scholar]

Associated Data

This section collects any data citations, data availability statements, or supplementary materials included in this article.

Supplementary Materials

Supplementary Figure S1

ABA-responsive gene expression in guard cells from cch. Expression level of ABA-responsible genes, RAB18 and RD29B in GCPs from cch and wild-type (Col-0) plants determined by real-time quantitative PCR. Transcript abundance of each gene was normalized to TUB2. GCPs were incubated in the presence or absence of 20 μM ABA for 1 h. Data represent means of three technical measurements with the standard deviation (SD).

Click here for additional data file. (2.1MB, ZIP)
Supplementary Figure S2

Typical epidermal fragments used in the present study. Epidermal fragments were obtained by blending rosette leaves and subsequent collection of material on 58-μm-pore-sized nylon mesh as described in the Materials and Methods. Scale bar = 50 μm.

Click here for additional data file. (2.1MB, ZIP)
Supplementary Figure S3

Effect of ABA on stomatal aperture of the rtl1 mutant. Epidermal fragments isolated from dark-adapted rtl1 and WT plants were illuminated with BL superimposed on the background RL (RL+BL) for 2.5 h. ABA (20 μM) was added to epidermal fragments 20 min before BL illumination commenced (RL+BL+ABA). As a control, the epidermal fragments were incubated in the dark for 2.5 h (Dk). The stomatal apertures in the abaxial epidermis was measured microscopically. The data represent the means of 25 measurements ± SDs. The experiment was repeated three times on different occasions with similar results.

Click here for additional data file. (2.1MB, ZIP)

Articles from Frontiers in Plant Science are provided here courtesy of Frontiers Media SA

RESOURCES