Mg-chelatase I subunit 1 and Mg-protoporphyrin IX methyltransferase affect the stomatal aperture in Arabidopsis thaliana
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To elucidate the molecular mechanisms of stomatal opening and closure, we performed a genetic screen using infrared thermography to isolate stomatal aperture mutants. We identified a mutant designated low temperature with open-stomata 1 (lost1), which exhibited reduced leaf temperature, wider stomatal aperture, and a pale green phenotype. Map-based analysis of the LOST1 locus revealed that the lost1 mutant resulted from a missense mutation in the Mg-chelatase I subunit 1 (CHLI1) gene, which encodes a subunit of the Mg-chelatase complex involved in chlorophyll synthesis. Transformation of the wild-type CHLI1 gene into lost1 complemented all lost1 phenotypes. Stomata in lost1 exhibited a partial ABA-insensitive phenotype similar to that of rtl1, a Mg-chelatase H subunit missense mutant. The Mg-protoporphyrin IX methyltransferase (CHLM) gene encodes a subsequent enzyme in the chlorophyll synthesis pathway. We examined stomatal movement in a CHLM knockdown mutant, chlm, and found that it also exhibited an ABA-insensitive phenotype. However, lost1 and chlm seedlings all showed normal expression of ABA-induced genes, such as RAB18 and RD29B, in response to ABA. These results suggest that the chlorophyll synthesis enzymes, Mg-chelatase complex and CHLM, specifically affect ABA signaling in the control of stomatal aperture and have no effect on ABA-induced gene expression.
KeywordsABA Arabidopsis thaliana Infrared thermography Mg-chelatase I subunit 1 Mg-protoporphyrin IX methyltransferase Stomatal guard cells
Stomatal pores in the plant epidermis, each surrounded by a pair of guard cells, regulate gas exchange between plants and the atmosphere to control processes such as CO2 uptake for photosynthesis and transpiration for water loss regulation (Shimazaki et al. 2007). Stomatal opening is induced by light, whereas stomatal closure is induced by the phytohormone abscisic acid (ABA), which is synthesized in response to drought stress (Assmann and Shimazaki 1999; Schroeder et al. 2001). ABA-induced stomatal closure is driven by an efflux of K+ from guard cells through outward-rectifying K+ channels in the plasma membrane. Activation of K+ channels requires depolarization of the plasma membrane; this depolarization is achieved mainly through anion channels in the plasma membrane (Joshi-Saha et al. 2011; Kim et al. 2010; Negi et al. 2008; Schroeder et al. 1987; Vahisalu et al. 2008).
Recently, the PYR/PYL/RCAR (Pyrabactin resistance/Pyrabactin resistance 1-like/Regulatory component of ABA receptor) family of proteins was identified as an ABA receptor in Arabidopsis thaliana and ABA recognition by PYR/PYL/RCAR family proteins was shown to activate SnRK2 family protein kinases through inactivation of the central negative regulator type 2C protein phosphatases (PP2Cs) (Cutler et al. 2010; Ma et al. 2009; Park et al. 2009; Santiago et al. 2009). A pyr1/pyl1/pyl2/pyl4 quadruple mutant exhibited strong ABA-insensitive phenotypes for seed germination, root growth, gene expression (Park et al. 2009), and stomatal opening and closing (Nishimura et al. 2010) indicating functional redundancy among the PYR/PYL/RCAR family proteins. ABA has been suggested to activate SLOW ANION CHANNEL-ASSOCIATED 1 (SLAC1), which is thought to be a slow-type anion channel (Negi et al. 2008; Vahisalu et al. 2008), via PYR/PYL/RCAR-PP2Cs-SnRK2 modules followed by depolarization of the plasma membrane (Geiger et al. 2009; Lee et al. 2009). In addition to PYR/PYL/RCAR, several candidate ABA receptors have been reported including the Mg-chelatase H subunit (CHLH) (Du et al. 2012; 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). However, it was also reported that CHLH is not an ABA receptor (Müller and Hansson 2009; Tsuzuki et al. 2011). Therefore, the question of whether CHLH indeed functions as an ABA receptor remains controversial. Likewise, GCR2 is also controversial (Klingler et al. 2010).
CHLH is a multifunctional protein involved in chlorophyll synthesis (Bollivar 2006; Masuda 2008), plastid-to-nucleus retrograde signaling (Mochizuki et al. 2001), and ABA signaling. In chlorophyll synthesis, CHLH functions as a subunit of Mg-chelatase consisting of three subunits I, D, and H that are encoded by the CHLI, CHLD, and CHLH genes, respectively. Mg-chelatase catalyzes the insertion of Mg2+ into protoporphyrin IX, which is the first step of the chlorophyll synthesis pathway after diverging from the tetrapyrrole biosynthesis pathway. In the next step, Mg-protoporphyrin IX is methylated by Mg-protoporphyrin IX methyltransferase (CHLM) and four subsequent catalytic reactions produce chlorophyll a (Bollivar 2006; Masuda 2008).
Recently, the rapid transpiration in detached leaves 1 (rtl1) mutant bearing a novel missense mutation in CHLH was isolated from ethyl methanesulfonate (EMS)-treated Arabidopsis thaliana using a screen for mutants with altered stomatal aperture (Tsuzuki et al. 2011). Stomatal movement in the rtl1 mutant was insensitive to ABA, but the effects of ABA on seed germination and root growth were normal. CHLI1, a major Mg-chelatase I subunit isoform in Arabidopsis (Huang and Li 2009), has also been reported to affect ABA signaling. Stomata of chli1, a knockout mutant of CHLI1, showed an ABA-insensitive phenotype (Tsuzuki et al. 2011). Du et al. (2012) also reported that the stomata of cs, a T-DNA insertion knockdown mutant of CHLI1 and CHLI-RNAi lines showed an ABA-insensitive phenotype. These results indicated that the Mg-chelatase complex, including CHLH and CHLI1, is likely to affect the ABA-signaling pathway in guard cells. However, the molecular mechanism by which CHLH and CHLI1 mediate ABA-signaling in guard cells remains largely unknown.
The molecular mechanisms of signaling pathways that control stomatal opening and closure are largely unknown. Several screens for stomatal aperture mutants using infrared thermography under drought, low or high CO2, or blue light-illumination conditions identified mutants that showed a reduced temperature phenotype due to wide stomatal aperture or an elevated temperature phenotype due to constricted stomatal aperture. These studies identified important components involved in the regulation of stomatal opening or closure such as OPEN STOMATA (OST) 1 and 2 (Merlot et al. 2002, 2007; Mustilli et al. 2002), HIGH LEAF TEMPERATURE 1 (HT1) (Hashimoto et al. 2006), SLAC1 (Negi et al. 2008), STOMATAL CARPENTER 1 (SCAP1) (Negi et al. 2013), BLUE LIGHT SIGNALING 1 (BLUS1) (Takemiya et al. 2013), and PROTON ATPASE TRANSLOCATION CONTROL 1 (PATROL1) (Hashimoto-Sugimoto et al. 2013) indicating that infrared thermography is a potent tool for identification of stomatal aperture mutants.
In this study, we performed a screen using infrared thermography under normal growth conditions to elucidate molecular mechanisms of stomatal opening and closure and isolated a mutant designated low temperature with open-stomata (lost) 1. The lost1 mutant had a novel missense mutation in the CHLI1 gene and exhibited a partial ABA-insensitive phenotype similar to that of a CHLH mutant. Moreover, we showed that a subsequent enzyme in chlorophyll synthesis, CHLM, also affects ABA signaling in the control of stomatal aperture. Our data suggest that chlorophyll synthesis enzymes may play an important role in ABA signaling in stomatal guard cells.
Materials and methods
Plant materials and growth conditions
All Arabidopsis (Arabidopsis thaliana) mutants, glabra1 (gl1), phototropin2-1 (phot2 mutant), chli1, chlm, npq2, gun2-1 and gun3-1 were in the Col background and were grown in soil under a 16-h fluorescent light (6:00 A.M. to 10:00 P.M.; 50 µmol m−2 s−1)/8-h dark cycle at 24 °C at a relative humidity of 55–70 % in a growth room (Kinoshita et al. 2001; Mochizuki et al. 2008). The T-DNA insertional mutants chli1 (SAIL_230_D11) and chlm (SALK_110265) were obtained from the Arabidopsis Biological Resource Center (ABRC, Columbus, OH, USA). Homozygous chli1 mutant plants were identified by PCR using the T-DNA left-border primer, LB1, and a CHLI1 gene-specific primer. Homozygous chlm mutant plants were identified by PCR using the T-DNA left border primer, LBb1.3, and a CHLM gene-specific primer. Primers are shown in Table S1.
Mutant screening using infrared thermography
Ten thousand phot2 (M1) seeds were treated with ethyl methanesulfonate (EMS; Sigma-Aldrich) and EMS-mutagenized M2 seeds were prepared as described previously (Lightner and Caspar 1998). Approximately 80 M2 plants were grown for 2–3 weeks in soil in each pot. Leaf temperatures of the mutants were measured in a growth room using a TVS-500EX infrared thermography instrument (NEC Avio Infrared Technologies Co., Ltd.) and analyzed with the Avio Thermography Studio software. Leaf temperature measurements were taken in the centers of the mature leaves (11–25 leaves/mutant line). Individual mutant candidates with a leaf temperature more than 1 °C below the temperatures of the leaves of surrounding plants were selected. The candidates were further selected by re-measurement of leaf temperature in the M3 generation. The selected mutants were grown for 4 weeks and subjected to stomatal aperture measurement. We isolated three cold mutants designated as low temperature with open-stomata (lost) 1, lost2, and lost3.
Identification of the lost1, lost2, and lost3 loci
To identify the mutant loci, we performed genetic mapping in the lost mutants. The mutants were crossed with plants of the Landsberg erecta (Ler) ecotype and F2 plants were obtained. F2 plants with visible mutant phenotypes including pale green leaves for lost1 and reduced leaf temperature, wilting, and dark-green rosette leaves for lost2 and lost3 were selected and genomic DNA was isolated from the individual mutant plants (13–20 plants/mutant). Genetic mapping was performed using simple sequence length polymorphism (SSLP) markers and cleaved amplified polymorphism (CAPS) markers.
Measurement of stomatal aperture
Stomatal aperture was measured as described previously (Inoue et al. 2008) with minor modifications. Fully expanded rosette leaves were harvested in the dark from 5 to 7-week-old plants. The leaves were blended in a Waring blender equipped with an MC1 mini container (Waring Commercial) in 35 mL of MilliQ water. The epidermal fragments were collected on nylon mesh and rinsed with MilliQ water. The epidermal tissues were incubated in basal buffer (5 mM MES-Bistrispropane, 50 mM KCl, and 0.1 mM CaCl2, pH 6.5) and were irradiated with red/blue mixed light [blue light (Stick-B-32; EYELA, Tokyo, Japan) at 10 µmol m−2 s−1 combined with background red light (LED-R; EYELA) at 50 µmol m−2 s−1] for 2.5 h at 24 °C in the presence of 1, 10, or 20 µM ABA or equal volumes of dimethyl sulfoxide (DMSO). Stomatal apertures were measured microscopically in the abaxial epidermis by focusing on the inner lips of stomata. All measurements of stomatal response to light were performed between 11:00 A.M. and 3:00 P.M. To measure the apertures under growth conditions, the epidermal fragments were isolated as described above at zeitgeber time (ZT) 5–9 and were immediately subjected to microscopic measurement.
Measurement of chlorophyll contents
The chlorophyll contents of rosette leaves from 5- to 6-week-old plants were determined as described previously (Tsuzuki et al. 2011).
Construction of plant transformation vector
To complement the lost1 mutant with the wild-type CHLI1 gene, we constructed a gene transfer vector bearing the genomic CHLI1 gene under the control of the native CHLI1 promoter. The genomic CHLI1 gene, extending from −1,063 to 2,576 bp of the genomic CHLI1 locus including 5′ and 3′ noncoding sequences, was amplified by PCR from wild-type (Col-0) genomic DNA using primers shown in Table S1. The amplified 3,639-bp DNA fragment was treated with EcoRI and cloned into the gene transfer vector pCAMBIA1300 using the EcoRI site. The resulting vector was verified by DNA sequencing.
Transformation of Arabidopsis
The gene transfer vector was introduced into the Agrobacterium tumefaciens strain GV3101 and used to transform the lost1 mutant (Clough and Bent 1998). The transformed plants were selected on MS plates containing 1 % (w/v) sucrose and 50 µg ml−1 hygromycin. Complementation testing was performed using independent homozygous transgenic lines from the T3 generation.
RT–PCR and quantitative RT–PCR
Expression of CHLI1 (At4g18480) and CHLM (At4g25080) in the lost1 and chlm mutants, respectively, was determined by RT–PCR. Total RNA was extracted from rosette leaves of four- to six-week-old plants using an RNeasy Plant Mini Kit (Qiagen, Valencia, CA, USA), according to the manufacturer’s instructions. First-strand cDNAs were synthesized from 0.4 to 1 µg of total RNA using a Takara PrimeScript II First Strand cDNA Synthesis Kit (Takara, Tokyo, Japan) with oligo(dT)12–18 primer. The cDNA fragments were amplified by PCR using specific primers. TUB2 (At5g62690) was amplified by PCR to serve as an internal standard.
We determine the expression of the CHLI1, CHLH (At5g13630), and CHLM genes in guard-cell protoplasts (GCPs) of wild type (Col-0) using RT–PCR. GCPs were isolated from 5-week-old Col-0 plants as described previously (Ueno et al. 2005). Total RNA was extracted and first strand cDNAs were prepared from the GCPs as described above. CHLI1, CHLM, CHLH, and TUB2 cDNAs were amplified by PCR using specific primers shown in Table S1.
We used quantitative RT–PCR to determine the expression of the ABA-responsive genes RAB18 (At5g66400) and RD29B (At5g52300) in response to ABA in phot2, lost1, wild type (Col-0), chli1, and chlm plants. Two-week-old seedlings were incubated in liquid MS medium (pH 5.8) containing 50 µM ABA or an equal volume of DMSO for 3 h at 24 °C under light (50 µmol m−2 s−1). Total RNA was extracted and first strand cDNAs were prepared from the ABA-treated plants as described above. Quantitative RT–PCR was performed using Power SYBR Green PCR Master Mix and a StepOne™ Real-Time PCR system (Applied Biosystems, Carlsbad, CA, USA), as reported previously (Takahashi et al. 2012). RAB18, RD29B, and TUB2 cDNAs were amplified by PCR using specific primers (Table S1). Relative quantification was performed using the comparative cycle threshold method and the relative amount of the amplified RAB18 or RD29B product was normalized to that of TUB2, which served as an internal control.
Immunoblotting was performed as described previously (Tsuzuki et al. 2011) with minor modifications. Rosette leaves were harvested from 6-week-old plants and ground in extraction buffer (50 mM MOPS-KOH, pH 7.5, 100 mM NaCl, 2.5 mM EDTA, 2 mM DTT, 1 mM phenylmethylsulfonyl fluoride, and 200 nM leupeptin) using a mortar and pestle. Fifty micrograms of protein were loaded onto a gel and separated by SDS–polyacrylamide gel electrophoresis. Polyclonal antibodies against CHLH (Tsuzuki et al. 2011) and monoclonal antibody against actin (Sigma-Aldrich) were used at a 3,000-fold dilution.
Isolation of stomatal aperture mutants by infrared thermography
lost2 and lost3 are ABA-deficient mutants
As shown in Fig. 1, lost2 and lost3 showed strong leaf temperature and stomatal aperture phenotypes. We performed map-based cloning of the LOST2 and LOST3 loci and found that the lost2 mutation was caused by a missense mutation (Gly169 to Asp) in the ABA DEFICIENT 2 (ABA2, At1g52340) gene, which encodes short-chain dehydrogenase/reductase. The lost3 mutation was due to a nonsense mutation (Gln575 to stop codon) in the ABA DEFICIENT 3 (ABA3, At1g16540) gene, which encodes molybdenum cofactor sulfurase (Fig. S1) (Nambara and Marion-Poll 2005). To determine if the lost2 and lost3 mutants were ABA-deficient mutants, we examined NaCl-tolerance during seed germination (Léon-Kloosterziel et al. 1996). Seeds of the control phot2 mutant did not germinate in the presence of 200 mM NaCl, but lost2 and lost3 seeds germinated as well as did seeds of the ABA-deficient mutant npq2 (aba1) (Niyogi et al. 1998) (Fig. S1e) indicating that lost2 and lost3 are likely to be ABA-deficient mutants. Note that aba2 and aba3 were isolated previously as mutants showing low temperature and open-stomata phenotypes using infrared thermography (Merlot et al. 2002) indicating that the screening approach used in this study is effective for the isolation of stomatal aperture mutants.
Low leaf temperature and open stomata phenotypes in lost1 leaves are caused by a missense mutation in CHLI1
Stomata of lost1 exhibit a partially ABA-insensitive phenotype
We also examined the expression of CHLI1 and CHLH in wild-type guard cell protoplasts (GCPs) by RT–PCR. As shown in Fig. 3b, CHLI1 and CHLH expression was detected in GCPs. Consistent with this, the available expression database, Arabidopsis eFP Browser, also indicates that CHLI1 and CHLH are expressed in guard cells. These results suggest that Mg-chelatase might affect ABA signaling within guard cells. Further investigations will be needed to clarify this by the complementation experiments using guard cell-specific promoter, such as GC1 (Kinoshita et al. 2011; Wang et al. 2014; Yang et al. 2008).
ABA induces expression of ABA-responsive genes in lost1
CHLM also affects ABA signaling
Mg-chelatase subunit and CHLM mutants accumulate CHLH protein in leaves
CHLH protein was reported to accumulate to high levels in CHLI1, CHLH, and CHLM mutants (Huang and Li 2009; Pontier et al. 2007; Tsuzuki et al. 2011). We examined the amount of CHLH protein in the leaves of the lost1, rtl1, chli1, and chlm mutants. Consistent with previous reports, all mutants showed high accumulation of CHLH protein (Fig. S5). The amount of CHLH protein in these mutants was four- to ten-fold higher than in control plants.
Infrared thermal imaging is a useful tool for isolation of stomatal aperture mutants (Merlot et al. 2002). In this study, we isolated three mutants that exhibited low leaf temperature and open stomata phenotypes. These mutants were designated low temperature with open-stomata (lost) 1, lost2, and lost3. The lost2 and lost3 mutants were deemed to be ABA-deficient mutants with mutations in the ABA2 and ABA3 genes, respectively (Figs.1, S1). The aba2 and aba3 mutants were isolated in a previous study using infrared thermography (Merlot et al. 2002) indicating that the screening approach used in this study is reliable.
The lost1 mutant contained an Arg219 to Lys missense mutation in Mg-chelatase I subunit 1 (CHLI1) and showed a partial ABA-insensitive phenotype for stomatal movement and reduced chlorophyll content. Furthermore, transformation of the wild-type CHLI1 gene into lost1 complemented these phenotypes (Fig. 2). These results indicate that CHLI1 is responsible for the lost1 phenotypes. Mg-chelatase consists of three subunits I, D, and H (Gibson et al. 1995; Willows et al. 1996). The Arabidopsis genome has two CHLI genes, CHLI1 and CHLI2, and CHLI1 is thought to be the major isoform of Mg-chelatase I subunits in Arabidopsis (Huang and Li 2009). CHLI1 belongs to the AAA+ (ATPases associated with various cellular activities)-family of ATPases and the ATPase activity drives the Mg insertion reaction (Masuda 2008). Arg219 is located close to an ATP-binding Walker B motif in CHLI1 (Fodje et al. 2001), thus the lost1 mutation affects Mg-chelatase activity suggesting that Mg-chelatase activity is important not only for chlorophyll synthesis but also for ABA signaling in guard cells.
ABA-induced expression of ABA-responsive genes, such as RD29A and MYB2, was inhibited in the leaves of CHLH knockdown mutants (Shen et al. 2006) suggesting that CHLH is a positive regulator for ABA-responsive genes. In contrast, a recent investigation indicated that CHLH mutants such as cch and rtl1 showed normal ABA-induced expression of the ABA-responsive RAB18 and RD29B genes in guard cells (Tsuzuki et al. 2013). Therefore, whether CHLH mediates ABA-induced expression of ABA-responsive genes remains controversial. In this study, we examined the effect of CHLI1 on ABA-induced expression of ABA-responsive genes in seedlings by quantitative RT-PCR and found that the CHLI1 mutants, lost1 and chli1, had no effect on ABA-induced expression of the ABA-responsive RAB18 and RD29B genes (Fig. 4). In addition, seed germination and root growth in the lost1 missense mutant showed normal ABA sensitivity as in the control phot2 (Fig. S3). Taken together, these results indicate that Mg-chelatase complex including CHLH and CHLI1 probably has no effect on ABA-induced expression of ABA-responsive genes or ABA-dependent inhibition of seed germination and root growth.
Mg-chelatase catalyzes the insertion of Mg2+ into protoporphyrin IX, which is the first step of the chlorophyll synthesis pathway after the branch point from the tetrapyrrole biosynthesis pathway. Therefore, we next examined whether Mg-protoporphyrin IX methyltransferase (CHLM), which is a subsequent enzyme in chlorophyll synthesis, is involved in the regulation of stomatal movement. Interestingly, chlm, a knockdown mutant of CHLM, also showed an ABA-insensitive phenotype for stomatal response (Fig. 5e). In addition, the chlm mutant showed normal ABA-induced expression of the ABA-responsive RAB18 and RD29B genes and ABA-dependent inhibition of seed germination and root growth (Figs. 5f, S3). Taken together, these results indicate that CHLM also specifically affects ABA signaling in stomatal movement but not in gene expression or seed germination and root growth. To our knowledge, this is the first evidence that CHLM affects ABA signaling in stomatal movement.
Interestingly, lost1, chli1, and chlm accumulated the endogenous CHLH protein (Fig. S5), but these mutants showed ABA-insensitive phenotype in stomatal movement (Figs. 3, S2a). On the other hand, CHLH overexpression in wild-type plants showed ABA-hypersensitive phenotype in stomatal movement (Tsuzuki et al. 2013). These results suggest that CHLH protein accumulation is not sufficient for complementation of the ABA-insensitive phenotype of these mutants, and that CHLI1 and CHLM may be required in addition to CHLH for a proper ABA response in stomatal movement. Further investigation will be needed to clarify whether CHLH over-accumulates in guard cells of these mutants, since the present data obtained from leaves (Fig. S5). CHLM antisense transgenic tobacco plants showed reduced Mg-chelatase activity (Alawady and Grimm 2005). Therefore, it is possible that decreased CHLM expression in the chlm-knockdown mutant affects ABA signaling by impairing Mg-chelatase activity. Further investigation is needed to clarify how CHLM affects ABA signaling via Mg-chelatase activity in guard cells. It is noteworthy that cytosolic Ca2+ is suggested to be important for the regulation of CHLH-mediated ABA signaling in guard cells (Tsuzuki et al. 2011). Therefore, further investigations of intercellular Ca2+ changes in guard cells of CHLH, CHLI1, and CHLM mutants will provide important information on the physiological role and molecular mechanism of CHLH, CHLI1, and CHLM in the ABA-signaling in stomatal guard cells.
Note that ch1-2, which is a loss-of-function mutant of chlorophyll a oxygenase converting from chlorophyll a to chlorophyll b showed normal ABA-response in stomatal movement (Shen et al. 2006). However, whether four enzymes (Mg-protoporphyrin IX monomethyl ester cyclase, 3,8 divinyl-protochlorophyllide 8 vinyl reductase, protochlorophyllide reductase, and chlorophyll synthase) subsequent to CHLM in the chlorophyll synthesis pathway from Mg-protoporphyrin IX monomethyl ester to chlorophyll a (Bollivar 2006; Masuda 2008) are involved in the regulation of stomatal movement is still unknown. Therefore, the effects of these four enzymes on stomatal movement should be examined.
Protoporphyrin IX is catalyzed not only by Mg-chelatase in the chlorophyll synthesis pathway, but also by the enzymes in phytochromobilin synthesis pathway (Mochizuki et al. 2010; Tanaka et al. 2011). It is possible that the phytochromobilin synthesis pathway also affects ABA-signaling in guard cells. Then, we examined stomatal phenotype in gun2-1 and gun3-1, mutants of heme oxygenase and phytochromobilin synthase in the phytochromobilin synthesis, respectively (Mochizuki et al. 2008). Interestingly, these mutants showed open-stomata and partial ABA-insensitive phenotypes (Fig. S2b). These results suggest that the phytochromobilin synthesis pathway also affects ABA-signaling in guard cells, although Shen et al. (2006) showed normal ABA-induced stomatal closure in gun2 and gun3 mutants. It should be noted that gun2-1 and gun3-1 mutants are phytochromobilin-deficient mutants and have no functional phytochromes (Parks and Quail 1991). However, it has been reported that phyB acts as a positive regulator for light-induced stomatal opening (Wang et al. 2010). Therefore, open-stomata phenotype in gun2-1 and gun3-1 is unlikely due to deficient of phytochromes. Further investigation will be needed to clarify how the phytochromobilin synthesis pathway affects ABA-signaling in guard cells.
We thank Dr. Takuya Matsuo (Nagoya University) for technical advice on measurement of ABA contents. This work was supported in part by Grants in Aid for Scientific Research (22119005 and 21227001) from the Ministry of Education, Culture, Sports, Science, and Technology (T.K.) and by the Advanced Low Carbon Technology Research and Development Programme from the Japan Science and Technology Agency (T.K.).
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