Mg-chelatase H subunit affects ABA signaling in stomatal guard cells, but is not an ABA receptor in Arabidopsis thaliana
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Mg-chelatase H subunit (CHLH) is a multifunctional protein involved in chlorophyll synthesis, plastid-to-nucleus retrograde signaling, and ABA perception. However, whether CHLH acts as an actual ABA receptor remains controversial. Here we present evidence that CHLH affects ABA signaling in stomatal guard cells but is not itself an ABA receptor. We screened ethyl methanesulfonate-treated Arabidopsis thaliana plants with a focus on stomatal aperture-dependent water loss in detached leaves and isolated a rapid transpiration in detached leaves 1 (rtl1) mutant that we identified as a novel missense mutant of CHLH. The rtl1 and CHLH RNAi plants showed phenotypes in which stomatal movements were insensitive to ABA, while the rtl1 phenotype showed normal sensitivity to ABA with respect to seed germination and root growth. ABA-binding analyses using 3H-labeled ABA revealed that recombinant CHLH did not bind ABA, but recombinant pyrabactin resistance 1, a reliable ABA receptor used as a control, showed specific binding. Moreover, we found that the rtl1 mutant showed ABA-induced stomatal closure when a high concentration of extracellular Ca2+ was present and that a knockout mutant of Mg-chelatase I subunit (chli1) showed the same ABA-insensitive phenotype as rtl1. These results suggest that the Mg-chelatase complex as a whole affects the ABA-signaling pathway for stomatal movements.
KeywordsABA Ca2+ Mg-chelatase H subunit Receptor Signal transduction Stomatal guard cell
In higher plants, the stomata, surrounded by pairs of guard cells, are the pores in the plant epidermis that regulate gas exchange between the leaves and the atmosphere. Opening of the stomata allows both transpiration and CO2 entry for photosynthesis. Under drought stress, the phytohormone abscisic acid (ABA) induces stomatal closure to prevent water loss (Schroeder et al. 2001; Shimazaki et al. 2007). ABA-induced stomatal closure is driven by an efflux of K+ from the guard cells through voltage-dependent outward-rectifying K+ channels in the plasma membranes. Activation of the K+ channels requires depolarization of the plasma membrane, and this depolarization is mainly achieved by the activation of anion channels within the plasma membrane (Schroeder et al. 1987; Kim et al. 2010).
Recently, the family of proteins containing pyrabactin resistance (PYR), pyrabactin resistance 1-like (PYL), and regulatory component of ABA receptor (RCAR) has been identified as a reliable family of ABA receptors, and ABA recognition by the PYR/PYL/RCAR family of proteins activates the SnRK2 family of protein kinases through inactivation of their central negative regulators, the type 2C protein phosphatases (PP2Cs) (Ma et al. 2009; Park et al. 2009; Santiago et al. 2009; Cutler et al. 2010). The pyr1 pyl1 pyl2 pyl4 quadruple mutant exhibited a phenotype with strong ABA-insensitive seed germination, root growth, gene expression (Park et al. 2009), and stomatal opening and closing responses (Nishimura et al. 2010), indicating a functional redundancy within the PYR/PYL/RCAR family proteins. More recently, SLAC1, which is thought to be a slow-type anion channel (Negi et al. 2008; Vahisalu et al. 2008), was shown to undergo phosphorylation via an SnRK2 family protein kinase and induce depolarization of the plasma membrane (Geiger et al. 2009; Lee et al. 2009). In addition to PYR/PYL/RCAR family proteins, several candidate ABA receptors have been reported, including the Mg-chelatase H subunit (CHLH) (Shen et al. 2006; Wu et al. 2009), G-protein coupled receptor 2 (GCR2) (Liu et al. 2007), and G-protein coupled receptor-type G proteins (GTG1 and GTG2) (Pandey et al. 2009). It should be noted that CHLH and GCR2, the ABA receptor candidates, have been controversially debated (McCourt and Creelman 2008; Cutler et al. 2010).
CHLH is one of the three subunits of Mg-chelatase (D, H, and I subunits). Mg-chelatase complex is involved in the biosynthetic pathway of chlorophyll, catalyzing the insertion of Mg2+ into protoporphyrin IX to form Mg-protoporphyrin IX (Gibson et al. 1995; Willows et al. 1996; Huang and Li 2009). CHLH has also been reported as genomes uncoupled 5 (GUN5), a regulator of plastid-to-nucleus retrograde signaling (Mochizuki et al. 2001). Furthermore, CHLH was identified as an ABA-specific binding protein in Vicia faba (Zhang et al. 2002). Subsequent extensive genetic and biochemical analyses using Arabidopsis suggested that CHLH specifically binds ABA and mediates ABA-signaling pathways involved in seed germination, root elongation, gene expression, and stomatal closure (Shen et al. 2006; Wu et al. 2009). More recently, knockout of a group of WRKY transcription factors (WRKY40, WRKY18, and WRKY60) in cch mutant has shown to rescue ABA-insensitive phenotypes of cch, including stomatal movements, seed germination and post-germination growth, suggesting that these WRKY transcription factors function as negative regulators of ABA signaling (Shang et al. 2010). The expression of CHLH is also suppressed by a key component of the circadian clock, TOC1, which interacts with the CHLH promoter; overexpression of TOC1 was shown to give rise to a phenotype with stomatal guard cells that were insensitive to ABA, as did also RNAi-mediated knockdown of CHLH (Legnaioli et al. 2009). In contrast, Müller and Hansson (2009) reported that recombinant Xan-F, an ortholog of CHLH in barley, did not bind ABA, and that xan-f loss-of-function mutants showed normal ABA responsiveness. Thus, whether CHLH functions as an ABA receptor remains controversial. Further investigations are required to elucidate the role of CHLH in ABA signaling.
Several secondary messengers regulate ABA signaling in stomatal guard cells, including Ca2+, reactive oxygen species, nitric oxide, phosphatidic acid, inositol derivatives, and sphingolipids (Kim et al. 2010). Of these, involvement of Ca2+ in ABA signaling has been well established. Cytosolic Ca2+ elevation and/or oscillation play an important role in ABA-induced stomatal closure (Allen et al. 1999, 2000, 2001; Islam et al. 2010). Treatment of the epidermis with Ca2+-chelating agents such as EGTA suppresses ABA-induced stomatal closure (Hwang and Lee 2001). These results suggest that Ca2+ acts as a signal mediator in ABA-induced stomatal closure. Moreover, the sensitivity of stomatal closing in response to elevations in the cytosolic Ca2+ concentration has been suggested to be enhanced (primed) by ABA (Young et al. 2006). A Ca2+-independent pathway in the ABA signaling of stomatal guard cells has also been reported (Allan et al. 1994; Marten et al. 2007; Siegel et al. 2009).
In the present study, we performed a screen focused on stomatal aperture-dependent transpiration in detached leaves from Arabidopsis thaliana that had been treated with ethyl methanesulfonate (EMS) to induce mutations. Consequently, we isolated a rapid transpiration in detached leaves 1 (rtl1) mutant in which the stomatal movements were insensitive to ABA, and which we identified as a novel missense mutant of the Mg-chelatase H subunit (CHLH). Phenotypic and ABA-binding analyses suggested that CHLH affects ABA signaling in stomatal movements but is not itself an ABA receptor. We propose a novel hypothesis regarding the role of CHLH in ABA signaling of stomatal guard cells.
Materials and methods
Plant materials and growth conditions
Arabidopsis thalianagl1 [Columbia (Col), carrying homozygous recessive gl1], used here as the wild type (WT), is the background ecotype of an rtl1 mutant. rtl1 was backcrossed with gl1 three times. Col is the background ecotype of a cch mutant (Mochizuki et al. 2001) and a T-DNA insertion mutant of CHLI1 (chli1; SAIL_230_D11). The transgenic line pOCA107-2 is the genetic background of a gun5-1 mutant (Mochizuki et al. 2001). The chli1 mutant was obtained from the Arabidopsis Biological Resource Center (Ohio State University, Columbus, OH, USA). Plants were grown in soil under 16-h fluorescent light (50 μmol m−2 s−1)/8-h dark cycle at 24°C in 55–70% humidity in a growth room.
To obtain the homozygous mutant line of chli1, the plant was identified by PCR using T-DNA left-border primer LB1 (5′-GCCTTTTCAGAAATGGATAAATAGCCTTGCTTCC-3′) and CHLI1 gene-specific primer (5′-GGAATCCAAATAAGGCCAAAG-3′).
Isolation of the rtl1 mutant and identification of the RTL1 locus
EMS-treated gl1 M2 seeds, purchased from Lehle Seeds (Round Rock, TX, USA), were germinated and grown under the same conditions as above. For the screening of leaf transpiration mutants, the fresh weight of a detached rosette leaf was measured at 0 and 90 min after detachment from each 4-week-old M2 plant. Individuals that showed a rapid or slow weight change compared to WT plants were selected as candidates for rapid-transpiration or slow-transpiration mutants, respectively. To determine stomatal phenotypes, we measured stomatal apertures in the isolated epidermis of 4-week-old candidate plants under several conditions using a microscope. With this screening strategy, we successfully isolated three rapid transpiration in detached leaves (rtl) mutants and two slow transpiration in detached leaves (stl) mutants.
To generate mapping populations, the rtl1 mutant was crossed with the Landsberg erecta (Ler) accession of A. thaliana. The rtl1 DNA was isolated from 143 F2 plants that showed a pale-green phenotype. DNA was isolated from individual mutant plants and mapping was performed using simple-sequence length polymorphism (SSLP) markers.
Vector construction for plant transformation
A genomic DNA fragment containing the CHLH gene, including its promoter region (from −2,814 to 5,748 bp of the CHLH locus; gCHLH), from WT plants was amplified by PCR using the specific primer set 5′-CAGCAGCCACGAGTCCTGATACAGCTCG-3′ and 5′-GTCTCGTGTCACGGCTACTGCAGATGAAGATG-3′. The amplified 8,562-bp DNA was cloned into the Gateway entry vector pCR8/GW/TOPO (Invitrogen, Carlsbad, CA, USA) and recombined by the LR reaction into the binary vector pGWB1 (Nakagawa et al. 2007). The resulting pGWB1-gCHLH vector was used to transform rtl1 plants for the complementation test. RNA interference (RNAi) lines with downregulated CHLH were generated as previously reported (Shen et al. 2006), with some modifications. A gene-specific 653-bp fragment, which was located 2,363–3,015 bp downstream from the start codon, was amplified by PCR using the primer pair 5′-ACAGAGATTCTGTGGTTGGGAAAG-3′ and 5′-GGCACTTGCCATTGCTGCTG-3′. The PCR product was introduced into pCR8/GW/TOPO and transferred into the binary vector pYU501 (Ueno et al. 2007). The resulting pYU501-CHLH RNAi was then used for transformation of WT plants. Transformation was performed using the GV3101 strain of Agrobacterium tumefaciens and the floral dip method (Clough and Bent 1998).
Measurement of stomatal aperture
Stomatal apertures were measured according to Inoue et al. (2008) with some modifications. The epidermal tissues isolated from dark-adapted 4- to 6-week-old plants were incubated in basal buffer (5 mM MES-BTP, pH 6.5, 50 mM KCl, and 0.1 mM CaCl2). For inhibition of light-induced stomatal opening by ABA, the epidermal tissues were incubated under blue/red light [blue light (Stick-B-32; EYELA, Tokyo, Japan) at 10 μmol m−2 s−1 superimposed on background red light (LED-R; EYELA) at 50 μmol m−2 s−1] for 2.5 h at 24°C in the presence or absence of 20 μM ABA. For the ABA-induced stomatal closure, the pre-illuminated epidermal tissues were incubated under blue/red light for 2.5 h with or without 20 μM ABA. Stomatal apertures in the abaxial epidermis were measured microscopically. Stomatal apertures are presented as the mean of 25 stomata with standard deviation (SD). Results were confirmed by blind reassessment by another researcher.
The total RNA was extracted from seedlings or leaves of 4- to 6-week-old plants using the RNeasy Plant Mini Kit (Qiagen, Valencia, CA, USA), according to the manufacturer’s instructions. First-strand cDNA was synthesized using the Takara PrimeScript II 1st Strand cDNA Synthesis Kit (Takara, Tokyo, Japan) and used as a template. A 741-bp fragment of CHLH cDNA was amplified using the primer pair 5′-GTGTGAGACCAATTGCTGATAC-3′ and 5′-ACTCCATCCCACAGTGTTGG-3′. A 952-bp fragment of CHLI1 cDNA was amplified using the primer pair 5′-GGAATCCAAATAAGGCCAAAG-3′ and 5′-ACCCATCAACATTGAGCTCTG-3′. TUB2 (At5g62690), used as a control, was amplified using the primer pair 5′-CATTGTTGATCTCTAAGATCCGTG-3′ and 5′-TACTGCTGAGAACCTCTTGAG-3′.
Immunoblot analysis was performed according to Hayashi et al. (2010) with modification. Seedlings or leaves from 4- to 6-week-old plants were ground in extraction buffer (50 mM MOPS–KOH, pH 7.5, 2.5 mM EDTA, 100 mM NaCl, 1 mM phenylmethylsulfonyl fluoride, 20 μM leupeptin, and 2 mM DTT) using a mortar and pestle. Fifty micrograms of protein was loaded and separated by SDS-polyacrylamide gel electrophoresis. To detect CHLH, the polyclonal antibody raised in rabbits against recombinant CHLH protein was used for immunoblot analysis. The 14-3-3 proteins were detected with the anti-14-3-3 protein (GF14ø) antibody (Kinoshita and Shimazaki 1999) as a control. The anti-CHLH and anti-14-3-3 protein antibodies were used at a 3,000-fold dilution.
Measurement of chlorophyll contents
The chlorophyll content of rosette leaves from 4-week-old plants was determined as previously described (Moran 1982).
Preparation of recombinant proteins
The coding sequences of CHLH (from 145 to 4,146 bp; At5g13630) and full-length PYR1 (At4g17870) and ABI1 (At4g26080) were amplified by PCR using cDNA prepared from WT plants. The primers used were the following: CHLH (5′-TCTGCTGTATCTGGAAACGGC-3′ and 5′-TTATCGATCGATCCCTTCGATCTTG-3′), PYR1 (5′-ATGCCTTCGGAGTTAACACC-3′ and 5′-TCACGTCACCTGAGAACCAC-3′), ABI1 (5′-ATGGAGGAAGTATCTCCGGC-3′ and 5′-TCAGTTCAAGGGTTTGCTCTTGAG-3′). The PCR products were initially cloned into pCR8/GW/TOPO and transferred into a pDEST17 destination vector containing a 6× His epitope-tag (Invitrogen) or into pDEST15 destination vector containing GST-tag (Invitrogen) by the LR reaction. Each construct was transformed into E. coli BL21 strains, and protein expression was induced by the addition of 0.1 mM isopropyl thiogalactoside, with overnight incubation at 30°C. Purification of recombinant His-tagged CHLH and PYR1 proteins was carried out using the His Bind Kit (Novagen, Madison, WI, USA) and Ni–NTA agarose (Qiagen). Purification of recombinant His-tagged ABI1 protein was performed by the same method as CHLH or PYR1, except that all buffers contained 5 mM MgCl2 (Melcher et al. 2009). The purified CHLH protein was used for the ABA-binding assay and as an antigen for preparing the anti-CHLH antibody. The recombinant GST-CHLH and GST-PYR1 proteins were purified with glutathione Sepharose 4B beads (GE Healthcare, Uppsala, Sweden). Protein concentrations were determined with the Bio-Rad protein assay kit using bovine serum albumin as a standard.
ABA binding to purified E. coli-expressed recombinant CHLH protein was assayed using 3H-labeled (±)-ABA (370 MBq μmol−1; American Radiolabeled Chemicals, Inc., St. Louis, MO, USA) by both the filter and pull-down methods.
For the filter method (Melcher et al. 2009; Wu et al. 2009), 2 μM purified His-tagged CHLH, PYR1, and ABI1 proteins and 50 nM 3H-labeled ABA were incubated in 0.2 mL binding buffer (10 mM Tris-Mes, pH 7.0, 2 mM MgCl2, 1 mM CaCl2, 1 mM DTT, and 250 mM mannitol) with or without 1,000-fold unlabeled ABA (no. A1049; Sigma, St. Louis, MO, USA) for 1 h at 25°C. The 3H-labeled ABA-bound protein was separated from free 3H-labeled ABA by filtering using GF/F glass fiber filter (Whatman, Little Chalfont, Buckinghamshire, UK) and washed with 5 mL ice-cold binding buffer three times. Then, the 3H-labeled ABA remaining on the filter was quantified using a liquid scintillation counter (LSC-5100; Aloka, Tokyo, Japan). PYR1 with ABI1 was used as a control of ABA binding.
For the pull-down method (Melcher et al. 2009), GST-CHLH (30 μg) or GST-PYR1 (4.3 μg) protein-bound glutathione Sepharose 4B beads and 50 nM 3H-labeled ABA were incubated in 0.2 mL binding buffer with or without 1,000-fold unlabeled ABA for 1 h at 25°C. For the binding assay of GST-PYR1, the reaction mixture were supplemented with the purified His-ABI1 (9.5 μg). Then, the beads were washed three times with the binding buffer and the radioactivity of the bound 3H-labeled ABA was measured using a liquid scintillation counter.
Seed germination and root growth assays
Seed germination and root growth assays were performed as previously reported (Shen et al. 2006). For the seed germination test, approximately 100 sterilized seeds were planted on a plate containing Murashige and Skoog inorganic salts (MS medium, pH 5.9), 3% sucrose, and 0.8% agar in the presence of 0 and 3 μM ABA. The plate was kept at 4°C for 3 days, then incubated at 24°C under fluorescent light (50 μmol m−2 s−1). The number of germinated seeds was determined at the indicated times after start of incubation. For the root growth assay, 4-day-old seedlings grown on a MS plate under fluorescent light were transferred to MS medium containing 0, 5, 10, or 20 μM ABA. After 7 days, the root length was measured.
An rtl1 mutant phenotype had stomatal guard cells that were insensitive to ABA
We then analyzed the stomatal responses of rtl1 in more detail. The WT stomata closed in darkness and opened when exposed to light, and this was inhibited by 20 μM ABA. Notably, the stomata of rtl1 plants opened moderately in darkness, and light-induced stomatal opening was not inhibited by ABA (Fig. 1c). Moreover, the rtl1 plants did not show ABA-induced stomatal closure (Fig. 1d). Thus, we suspected that rapid transpiration phenotype of rtl1 is likely due to insensitivity to ABA after detachment of rosette leaves since stomatal aperture under light condition in rtl1 is almost same with that in wild type (Fig. 1c, d). In addition, seed germination and root growth showed normal ABA sensitivities in the rtl1 plants (Fig. S1). These results indicate that the ABA-insensitive phenotype of rtl1 is specific to stomatal movements.
A missense mutation of CHLH was responsible for the ABA-insensitive rtl1 phenotype
To confirm these results, we prepared CHLH knockdown plants. Because T-DNA insertion mutants in the CHLH gene are lethal (Shen et al. 2006), we instead prepared CHLH RNAi plants, which exhibited lower amounts of the CHLH transcript and CHLH protein (Fig. 3a, b). The CHLH RNAi plants exhibited a semi-dwarf and pale-green phenotype and did not show ABA-induced stomatal closure (Fig. 3c–e). The CHLH missense mutant, cch (P642 to L), also demonstrated ABA insensitivity, but another CHLH missense mutant, gun5-1 (A990 to V), showed normal ABA-induced stomatal closure (Fig. 2f), consistent with a previous report (Shen et al. 2006). The ABA sensitivities of seed germination and root growth were normal in both cch and rtl1 plants under our growth conditions (Fig. S1). Taken together, these results suggest that CHLH plays a role in the ABA-signaling pathway involved in stomatal movements.
Recombinant CHLH did not bind ABA
Note that in our assays, we could not detect binding of ABA to PYR1 alone, and ABA binding by PYR1 required the presence of ABI1 (Fig. 4c). In accord with this finding, the ABA-binding affinity of PYL5 and RCAR1/PYL9 was reported to increase more than tenfold in the presence of PP2Cs (e.g., HAB1 and ABI2) (Ma et al. 2009; Santiago et al. 2009).
High concentration of extracellular Ca2+ restored ABA responsiveness of rtl1 stomata
A chli1 knockout mutant also had an ABA-insensitive phenotype
A screen focused on stomata aperture-dependent water loss via transpiration
One powerful tool for identifying signaling components of stomatal opening and closing is the generation of mutants that show impaired stomatal movements. However, direct microscopic measurement of stomatal apertures is difficult with a large number of plants. Mustilli et al. (2002) reported that the open-stomata mutants, ost1-1 and ost1-2, which were isolated by thermal imaging, exhibit a high rate of water loss via transpiration in their detached leaves. Therefore, measurement of weight changes in detached leaves is an effective method to identify stomatal-aperture mutants. Here, we performed a screen focused on stomatal aperture-dependent water loss in EMS-treated Arabidopsis by weighing detached leaves with a microbalance and successfully isolated three rtl and two stl mutants. To our knowledge, this is the first report of stomatal aperture mutants isolated by this method.
CHLH affects the ABA-signaling pathway in guard cells but is not itself an ABA receptor
Previous reports have suggested that CHLH localized in chloroplasts is an ABA receptor, and that the known missense mutant, cch, has a phenotype that is ABA-insensitive in seed germination, root growth, gene expression, and stomatal movements (Shen et al. 2006; Wu et al. 2009). It should be noted that at the beginning CHLH was identified as an ABA-binding protein using ABA-immobilized at its carboxylate on an affinity resin (Zhang et al. 2002). Given that carboxylate in ABA is needed for bioactivity, this approach potentially possessed a problem (Cutler et al. 2010). In the present study, we could not detect ABA binding to recombinant CHLH protein using 3H-labeled ABA (Fig. 4), and we found no evidence of ABA resistance in either seed germination or root growth in the cch and rtl1 mutants (Fig. S1), even though we performed these experiments in accordance with reported methods (Shen et al. 2006; Melcher et al. 2009; Wu et al. 2009). In contrast, however, the CHLH missense mutants, cch and rtl1 (Figs. 1, 2), as well as CHLH RNAi plants (Fig. 3), showed ABA-insensitive stomatal movements, in agreement with previous reports (Shen et al. 2006; Wu et al. 2009). From these results, we conclude that CHLH specifically affects ABA signaling in guard cells but is not itself an ABA receptor.
The rtl1 mutation is a single nucleotide substitution (C2068 to T), leading to a missense mutation in the protein (L690 to F) (Fig. 2). The missense mutation of cch (P642 to L) is proximally close to that of rtl1, and indeed, both mutants have nearly identical phenotypes. In contrast to these, the missense mutation of gun5-1 (A990 to V), whose phenotype is ABA-sensitive (Shen et al. 2006), is relatively distant from the rtl1 and cch mutations. These results suggest that the region around the rtl1 and cch mutations is important for ABA responsiveness in stomatal guard cells, and that the region around gun5-1 mutation has no effect on the ABA responsiveness. In addition, the loss-of-function mutant, xan-f10, a mutant of Xan-F10 that is an ortholog of CHLH in barley, showed normal ABA responsiveness (Müller and Hansson 2009). However, the mutation of xan-f10 is a 3-bp deletion that removes the conserved amino acid residue E424, suggesting that the region around the xan-f10 mutation has no effect on the ABA responsiveness of stomatal guard cells.
We observed significant stomatal closure in the CHLH missense mutant, rtl1, when ABA was applied simultaneously with a high extracellular concentration of Ca2+ (Fig. 5). Therefore, the CHLH missense mutations of cch and rtl1 may depress Ca2+ mobilization from intracellular Ca2+ stores in response to ABA, thereby damping the cytosolic Ca2+ elevation and/or oscillation in stomatal guard cells. Moreover, these results suggest that chloroplasts may have a crucial role for Ca2+ mobilization since CHLH is a chloroplast-localized protein. It is worthy of note that an important role of chloroplasts for Ca2+ signaling in guard cells has been reported (Nomura et al. 2008; Weinl et al. 2008). Further investigations will be needed to examine intracellular Ca2+ changes in response to ABA in guard cells of rtl1 in the presence and absence of a high concentration of extracellular Ca2+.
Mg-chelatase complex plays an indirect role in ABA signaling in guard cells
Mg-chelatase is a complex enzyme of three subunits, H, D, and I, and all subunits are required for Mg-chelatase activity in chlorophyll biosynthesis (Gibson et al. 1995; Willows et al. 1996; Huang and Li 2009). Our results indicate that not only CHLH missense mutants, but also a CHLI1 knockout mutant, showed ABA insensitivity of stomatal movements (Fig. 6). Therefore, the Mg-chelatase complex as a whole probably affects the ABA-signaling pathway in stomatal guard cells. In addition, Mg-protoporphyrin IX may be involved in the regulation of the ABA signaling in guard cells, since Mg-chelatase complex is Mg-protoporphyrin IX-producing enzyme (Matsuda 2008). Further investigation will be needed to clarify this.
Note that GUN4 is shown to stimulate the activity of Mg-chelatase (Larkin et al. 2003). It is worthy to examine whether GUN4 is involved in ABA signaling in stomatal guard cells, although gun4-1, a missense mutant (Larkin et al. 2003), did not show ABA-insensitive phenotype (Shen et al. 2006).
A possible physiological role of CHLH in the ABA-signaling pathway in guard cells
In the CHLH RNAi experiments, the expression level of CHLH affected the ABA sensitivity of the stomatal guard cells (Fig. 3). This observation is consistent with a report stating that overexpression of a key circadian clock component, TOC1, which interacts with the CHLH promoter and suppresses expression of CHLH, gave rise to a phenotype in which stomatal guard cells were ABA-insensitive (Legnaioli et al. 2009). Taken together, these observations suggest that expression level of CHLH affects the ABA sensitivity of stomatal guard cells. Further investigations of diurnal changes of CHLH expression in guard cells and effects of drought stress on CHLH expression will provide important information on the physiological role of CHLH in the ABA-signaling pathway of stomatal guard cells.
We thank M. Goto and A. Takaki for their technical support. The cch, gun5-1, and pOCA107-2 were kindly provided by Dr. N. Mochizuki (Kyoto University). This work was supported in part by Grants-in-Aid for Scientific Research (20370021, 22119005, and 21227001) from the Ministry of Education, Culture, Sports, Science and Technology, Japan (T.K.) and by ALCA from the Japan Society for the Promotion of Science (T.K.).
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