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First published online August 12, 2004; 10.1105/tpc.104.022608 © 2004 American Society of Plant Biologists
Evidence for a Direct Link between Glutathione Biosynthesis and Stress Defense Gene Expression in Arabidopsis
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ABSTRACT |
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 TOP ABSTRACT INTRODUCTIONRESULTSDISCUSSIONMETHODSREFERENCES |
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50% lowered foliar glutathione levels. Mapping revealed that rax1-1 is an allele of 
-GLUTAMYLCYSTEINE SYNTHETASE 1 (GSH1), which encodes chloroplastic -glutamylcysteine synthetase, the controlling step of glutathione biosynthesis. By comparison of rax1-1 with the GSH1 mutant cadmium hypersensitive 2, the expression of 32 stress-responsive genes was shown to be responsive to changed glutathione metabolism. Under photo-oxidative stress conditions, the expression of a wider set of defense-related genes was altered in the mutants. In wild-type plants, glutathione metabolism may play a key role in determining the degree of expression of defense genes controlled by several signaling pathways both before and during stress. This control may reflect the physiological state of the plant at the time of the onset of an environmental challenge and suggests that changes in glutathione metabolism may be one means of integrating the function of several signaling pathways. |
INTRODUCTION |
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TOPABSTRACTINTRODUCTIONRESULTSDISCUSSIONMETHODSREFERENCES |
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; Ort and Baker, 2002). Although these processes are protective, they lead to increased formation of reactive oxygen species (ROS), such as superoxide anion (
), singlet O2, and hydrogen peroxide (H2O2; Asada, 1999). The prevention of oxidative stress is achieved by a network of low molecular weight antioxidants, enzymes that keep them reduced, and ROS-scavenging enzymes (Karpinski et al., 1997; Asada, 1999). The accumulation of ROS also activates defense gene expression as part of protective responses to both biotic and abiotic stimuli (Karpinski et al., 1999; Grant and Loake, 2000; Fryer et al., 2003; op den Camp et al., 2003). Transcript profiling studies, in some cases using transgenic plants altered in expression of antioxidant enzymes, indicate that coordinated regulation of a network of defense and antioxidant systems occurs (Willekens et al., 1997; Rossel et al., 2002; Pneuli et al., 2003).
A key component of the antioxidant network is the thiol glutathione, which is synthesized from its constituent amino acids, L-Glu, L-Cys, and Gly, in an ATP-dependent two-step pathway catalyzed by the enzymes -glutamylcysteine synthetase ([-ECS]; EC 6.3.2.2) and glutathione synthetase (EC 6.3.2.3), respectively (Noctor et al., 2002). To date, two genes, one coding for plastidial -ECS (GSH1) and one putative cytosolic glutathione synthetase (GSH2), have been identified in Arabidopsis thaliana and many other plant species (May and Leaver, 1993;; Rawlins et al., 1995; Cobbett et al., 1998; Noctor et al., 2002). Overexpression or inhibition of GSH1 expression causes Arabidopsis to have enhanced or depressed levels of glutathione, respectively (Cobbett et al., 1998; Xiang and Oliver, 1998; Vernoux et al., 2000). In keeping with studies on -ECS from other organisms, the plant enzyme is considered to be a key regulatory step in glutathione biosynthesis and may be controlled at the level of enzyme activity, synthesis of protein and mRNA (Xiang and Oliver, 1998; Noctor et al., 2002).
Glutathione, primarily in its reduced form (GSH), is present at concentrations of 2 to 3 mM in various plant tissues (Creissen et al., 1999; Meyer and Fricker, 2002; Noctor et al., 2002). Because glutathione is a major cellular antioxidant, it is regarded as a determinant of cellular redox state and may indirectly have an influence on many fundamental cellular processes (Cooper et al., 2002; Noctor et al., 2002; Schafer and Buettner, 2001). Glutathione can engage in thiol-disulphide exchange reactions that may be a key process in linking the regulation of gene expression to the redox state of cells or specific subcellular compartments (Schafer and Buettner, 2001; Noctor et al., 2002). In plants, the number of regulatory processes that are known to be potentially influenced by the levels or redox state of cellular glutathione pools is small. The regulation of plastid gene expression by the redox state of the glutathione pool provide the best studied examples to date. These include the translation of rbcL mRNA, the processing of specific plastid-encoded transcripts, and the modulation of RNA polymerase by a redox-sensitive protein kinase (Irihimovitch and Shapira, 2000; Pfannschmidt, 2003). Not many examples exist that have indicated the possibility of glutathione redox-mediated control of nuclear-located defense gene expression. Glutathione may activate the regulatory proteins NPR1 and possibly protein phosphatase 2C (ABI2), important in salicylic acid (SA) and abscisic acid (ABA) signaling, respectively (Meinhard et al., 2002; Mou et al., 2003). Earlier studies in which glutathione was fed to cells or leaves has been shown to both induce and suppress expression of a range of defense genes (Wingsle and Karpinski, 1996; Karpinski et al., 1997, 2000; Wingate et al., 1988; Loyall et al., 2000). However, given the many aspects of cellular metabolism that glutathione is engaged in (Noctor et al., 2002), such feeding data do not constitute evidence for a direct role in the regulation of antioxidant defense genes.
Under nonstress conditions, ASCORBATE PEROXIDASE2 (APX2), which encodes a component of the antioxidant network, is expressed at extremely low levels. However, when leaves are subjected to excess light or wounding that induces photo-oxidative stress, the expression of the gene is rapidly induced in bundle sheath tissue (Karpinski et al., 1997, 1999; Fryer et al., 2003; Chang et al., 2004). In this study, it is shown that the mutant regulator of APX2 1-1 (rax1-1), which expresses APX2 in the absence of excess light or wounding stress, is a lesion in GSH1. Thus, a direct link was established between expression of an antioxidant defense gene under steady state (nonstressed conditions) and glutathione. Further analysis of gene expression showed that only stress defense genes were affected by glutathione, ruling out wider effects of this mutation on cellular metabolism. Comparison of expression profiles under high light stress and wounding in rax1-1 and cadmium hypersensitive 2-1 (cad2-1, another mutant in GSH1; Cobbett et al., 1998) revealed unexpected differences despite similar gluthathione levels. From these data, it is deduced that both glutathione metabolism and levels can be considered to influence the poising of cellular defences before their induction as well as the actual response to an external stress.
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RESULTS |
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TOPABSTRACTINTRODUCTIONRESULTSDISCUSSIONMETHODSREFERENCES |
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) was chemically mutagenized and used to screen for APX2 expression in the absence of excess light stress (see Methods). After screening, two mutants were identified that had a stable, heritable luciferase-positive phenotype (example in Figure 1A). The mutant lines were visually indistinguishable from wild-type plants at all stages of their life cycle under both long (18-h photoperiod) and short (8-h photoperiod) day conditions. All data presented here are from selfed progeny of the fifth backcrossed generation. We have assigned only a single allele number to the mutants and refer to them in this article as rax1-1. This is because subsequent sequencing of the mutant loci revealed that the lesion was the same in both mutants (see below).
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Depressed Glutathione Levels in rax1-1
Under nonstress conditions, there was no effect of rax1-1 on the foliar levels of H2O2, lipid peroxidation products, and the levels or redox state of ascorbate and photosynthetic electron transport (data not shown). However, rax1-1 had 20 to 50% of the foliar level of glutathione compared with wild-type plants over a range of plant ages, irrespective of the photoperiod (Table 1). There was no effect on glutathione redox states at any of the stages of vegetative growth (data not shown). By contrast, foliar levels of Cys and -glutamylcysteine (-EC) were similar in rax1-1 and wild-type plants (Table 1). The levels of glutathione in rax1-1 were similar to that reported for cad2-1. However, in contrast with rax1-1 and wild-type plants, -EC was not detectable, and Cys levels were 37 to 70% higher in cad2-1 (Table 1). As in cad2-1 (Cobbett et al., 1998), -ECS activity was lower in rax1-1 compared with wild-type plants (rax1-1: 3.3 nmols -EC formed min–1 g fwt–1 [SD ± 0.3; n = 3], Col-0/APX2LUC 13.7 nmols -EC formed min–1 g fwt–1 [SD ± 2.5; n = 3])
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2 = 0.066, based on cosegregation of a recessive rax1-1 locus and a APX2LUC dominant transgene [13:3]). Mapping of the rax1-1 mutation using 48 F2 progeny displaying the mutant phenotype showed it was on chromosome 4 located between the FCA6 locus and BAC clone F28M11. This interval also harbors GSH1 (At4g23100). Because rax1-1 plants had lower levels of glutathione and -ECS activity, similar to cad2-1 (Table 1), we reasoned that rax1-1 could also be a GSH1 mutation. Therefore, the genes and cDNAs encoding GSH1 from both mutant types were sequenced. For both mutant types at the time considered to be different alleles of the same locus, sequencing revealed a point mutation (G to A) at coordinate 12,105,389 of the chromosome 4 sequence (The Arabidopsis Information Resource [TAIR], www.arabidopsis.org, November 2003). This coordinate is equivalent to coordinate 2883 of the sequence published by Cobbett et al. (1998) (EMBL: AF068299). This mutation was in exon 6 of GSH1 and resulted in an Arg (R229) to Lys (K) change in the -ECS sequence (Figure 1C). This Arg residue is conserved in the putative -ECS sequences from eight plant species (Figure 1C). In addition to the point mutation at coordinate 12,105,389, one of the mutant types had an additional point mutation (A to G) at coordinate 12,105,405. This second mutation produced no change in the sequence of -ECS (data not shown) but provided confirmation that both mutants arose independently from the screening but were the same allele.
To confirm that rax1-1 was a GSH1 mutant allele, crosses were done with cad2-1 plants and also a transgenic line expressing a GSH1 cDNA under the control of the Cauliflower mosaic virus 35S promoter (Xiang et al., 2001). The rax1-1 and cad2-1 mutants failed to complement one another because glutathione levels were not restored to wild-type levels in F1 progeny arising from a cad2-1 x rax1-1 cross (Table 2). Equally, the rax1-1 phenotype was abolished in homozygous rax1-1 individuals also harboring the 35S:GSH1 cDNA fusion in that glutathione levels were restored to wild-type levels (Table 2), and this was associated with a loss of luciferase activity from APX2LUC (data not shown). Therefore, we concluded that the lesion in GSH1 is the cause for the rax1-1 phenotype.
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To determine if the observed transcript changes resulted in changes in the activities of ROS-scavenging enzymes, the activities of Fe- and Cu/Zn- amd Mn-superoxide dismutase (SOD) isoforms, monodehydroascorbate reductase (MDAR), and cytosolic ascorbate peroxidase ([APX]; Figure 3) were determined in the nonstressed mutant and wild-type plants. Whereas total SOD activity was not significantly changed in rax1-1 and cad2-1 compared with wild-type plants, the proportion of Fe-SOD activity was increased from 27% of the total in wild-type plants to 
45% in both mutants (Figure 3A; P < 0.01). Similarly, Cu/Zn SOD activity was a lower proportion of total activity in both mutants (40%; P < 0.01 for rax1-1 and P < 0.05 for cad2-1) compared with wild-type plants (60%). Total MDAR activity was elevated above the wild-type level in both mutants (Figure 3B), whereas an increase in the activity of cytosolic APX was observed only in rax1-1, but not cad2-1, compared with the wild type (Figure 3C). These data on enzyme activities broadly agreed with the observed changes in transcript levels.
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8500 Arabidopsis genes was performed using microarrays (Zhu and Wang, 2000). A stringent analysis of the data (see Methods) cut the number of genes whose expression could be compared with wild-type plants down to 3743 and 3734 for rax1-1 and cad2-1, respectively. Pairwise comparisons between these reduced data sets from wild-type plants were conducted in turn with those from cad2-1 and rax1-1. Only genes that showed more than twofold differences in signal intensities between mutants and the wild type were classified as differentially expressed and analyzed further. We reasoned that genes whose expression was affected by a depressed level of foliar glutathione would be affected in the same way in rax1-1 and cad2-1, and these were observed (At1g65400, At4g02330, At2g05380, At4g39640, At4g21830, At2g24850, At5g24780, At5g24770, At2g14610, At3g57260, At2g43570, At2g48110, and At4g35580; Table 3). More surprisingly, two further groups could be discerned: seven genes whose expression was only altered in rax1-1 (At2g40300, At5g01600, At2g29580, At3g51860, At2g32880, At5g66400, and At2g46680; Table 3) and 206 genes with altered transcript level only in cad2-1 (see Supplemental Table 1S online). The transcript levels of five of the genes listed in Table 3 were analyzed by a quantitative RT-PCR (qRT-PCR) procedure. This showed that the patterns of expression of these genes in the mutants versus wild-type plants was the same as observed in the microarray experiment, although the absolute values differed between the two methods (Table 3, numbers in parentheses).
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Expression of APX2 and Other Defense Genes in rax1-1 and cad2-1 Leaves Subjected to Stress
When rax1-1 plants were subjected to excess light stress or wounding, induction of APX2 transcript was much more pronounced than in control plants (Figures 4A and 4B). qRT-PCR confirmed that APX2 expression after excess light stress was twofold to threefold higher in rax1-1 compared with wild-type plants and also in cad2-1 plants (Figure 5B). For cad2-1, this was despite the unaffected very low level of this transcript in low light conditions (Figure 2A). Furthermore, APX2 transcript levels in rax1-1, after a 1-h exposure to fivefold excess light stress, were still detectable 1 h after the stress, when levels in the wild-type plants had returned to below the level of detection (Figure 5A).
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Whole Plant Responses to Excess Light Stress and Bacterial Infection
The exposure of rax1-1 or cad2-1 plants to excess light did not produce any difference, when compared with parental plants, in any chlorophyll a fluorescence parameter used to measure different aspects of the efficiency of photosynthetic electron transport (see Supplemental Figure 3S online). Active photosynthetic electron transport is required for APX2 expression in excess light-stressed wild-type plants, but this was not the reason for the elevated APX2 expression in excess light stressed rax1-1 plants (Karpinski et al., 1997, 1999; Fryer et al., 2003). Whereas H2O2 levels increased in excess light-stressed plants, the mutants showed no differences compared with the wild type (data not shown). Similarly, the pattern of change in both glutathione redox state and levels in response to excess light was not different from the wild type, although the mutants always had lowered glutathione levels (data not shown). The decreased levels of transcripts involved in resistance to pathogens (Table 3) prompted us to test if the response to infection was compromised in the mutants. Both rax1-1 and cad2-1 showed weaker resistance to avirulent Pseudomonas syringae infection (Figure 6).
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DISCUSSION |
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TOPABSTRACTINTRODUCTIONRESULTSDISCUSSIONMETHODSREFERENCES |
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; De Vos et al., 1992; Walker and McKersie, 1993; Chaumont et al., 1995; Kampfenkel et al., 1995; Iturbe-Ormataexe et al., 1998; Brüggemann et al., 1999; Hernandez et al., 2000; Nikiforova et al., 2003). These lowered glutathione levels were accompanied by changes in many components of the antioxidant/ROS-scavenging network. Thus, despite the emphasis often given to glutathione (May et al., 1996; Allan and Fluhr, 1997; Noctor et al., 2002), there is no compelling evidence from these comparative studies that glutathione or any other single antioxidant could play a unique role in the regulation of antioxidant defenses. The isolation of rax1-1 by screening for APX2 expression under normal growth conditions and demonstrating that it is a lesion in GSH1 with reduced glutathione levels is an important observation. The way this mutant was identified provides direct evidence that glutathione metabolism and the expression of other components of plant antioxidant defenses are tightly linked.
The increased oxidation or lowered levels of cellular glutathione pools caused by different environmental conditions may constitute a signal that is mimicked by the permanently lowered levels of glutathione in rax1-1 and cad2-1 (Table 1). This is because the glutathione redox couple (2GSH 
GSSG + 2H+), unlike those of other antioxidants, is such that its redox potential can be determined by the concentration of GSH as well as the GSH/GSSG ratio (Schafer and Buettner, 2001; Pfannschmidt, 2003). This means that the GSH concentration alone can have an influence on cellular redox state and possibly influence redox-sensitive regulators (Schafer and Buettner, 2001; Noctor et al., 2002). This concept is sometimes referred to as redox tone (Cooper et al., 2002). Therefore, we reasoned that the level of glutathione common to cad2-1 and rax1-1 might permit identification of genes sensitive to cellular redox state. This was the case for the transcript levels and enzyme activity of three (out of 25) antioxidant defense genes surveyed (those encoding Fe- and Cu/Zn-SOD and MDAR; Figures 2 and 3) and a further 16 genes (out of 3743) from a microarray analysis (Table 3).
Surprisingly, the lowered level of glutathione per se did not provide an explanation for all of our observations. It was possible to identify genes whose transcript levels were specifically affected in rax1-1 or cad2-1 (Figure 2, Table 3; see Supplemental Table 1S online). The expression of 10 genes, including three antioxidant genes, most notably APX2 itself, but also DHAR1 and APX1, were affected in rax1-1 but not in cad2-1 (Figure 2, Table 3). The rax1-1 mutant had near wild-type levels of -EC, Cys (Table 1), Ser, Gly, and Glu (Ball, 2001), thus ruling out the levels of these compounds as possible additional effectors of expression of this group of genes. The discrepancy between rax1-1 and cad2-1 in the levels of thiol intermediates (Table 1) suggests that some other aspect of glutathione biosynthesis, besides its level, may be contributing to the regulation of defense gene expression in these plants. The distinct cad2-1 group of genes did not permit further analysis of this problem because the mutant had too many variables, such as elevated Cys levels, undetectable levels of -EC (Table 1), and possibly perturbed amino acid metabolism. root meristemless 1 (rml1) is a mutant allele of GSH1 (Figure 1C) that has 5% of wild-type glutathione levels and is severely defective in root growth (Vernoux et al., 2000). However, transgenic lines harboring antisense GSH1 display a similar reduced level of glutathione to rml1 and yet do not have such a severe phenotype (Xiang et al., 2001), perhaps reflecting subtle effects of altered glutathione metabolism on gene expression.
The differences in stress defense gene expression profiles between rax1-1 and cad2-1 may also suggest that the different lesions could have affected regulatory as well as catalytic functions of -ECS. Inspection of the position of the lesions in the GSH1 mutants adds some support to this notion. Both the cad2-1 and rml1-1 lesions lie within a putative catalytic domain of -ECS, as defined by a block of distant homology to trypanosome -ECS (Figure 1C; Leuder and Phillips, 1996). By contrast, the rax1-1 lesion lies outside this domain (Figure 1C), which may suggest that the effect of this mutation may be on a function not directly associated with the catalytic function of the enzyme. It should be noted that -ECS from plants shows a high degree of sequence conservation over the full length of the mature polypeptide (Noctor et al., 2002), which suggests that functions apart from the catalytic activity might be important in this enzyme.
Further evidence that glutathione biosynthesis, or the action of specific regions of GSH1, may influence stress protective gene expression in subtle ways comes from the results of our screen of M2 plants equivalent to 17,000 M1 individuals. If a perturbation in ROS homeostasis was solely responsible for enhanced APX2 expression, then it would have been expected to have recovered mutants that had diminished levels of other foliar antioxidants (e.g., similar to vtc-1 and npq1-2; Conklin et al., 1996; Niyogi et al., 1998). Furthermore, if depressed glutathione levels alone were the main influence on APX2 expression, we would have expected to, but did not recover, a wider range of GSH1 mutant alleles (for example, equivalent to cad2-1). In support of these conclusions, neither vtc1-1, npq1-2, or cad2-1 under nonstress conditions showed detectable APX2 expression (Figure 2A; Ball, 2001). In addition, rax1-1 did not show any increase in total foliar H2O2 levels or increases specifically in vascular tissue that would have explained the increased expression of APX2 (see Results; Fryer et al., 2003).
Under Nonstress Conditions, Glutathione Metabolism Affects a Group of Genes Functionally Clustered around Stress Defense
All of the known genes that showed altered expression in the microarray comparison between nonstessed rax1-1 and the wild type have been reported in the literature to be also responsive to stress, important as host factors in disease, or implicated in stress defenses in plants (Table 4; 24/26). Two more genes (At2g29580 and At4g35750) have homologs that have been implicated in stress responses in animal cells (Table 4). Interestingly, 8 of the 17 genes with depressed levels of transcripts in rax1-1 compared with the wild type (Table 3) have been shown to be altered in their expression by either ABA (three; Table 4), SA (two; Table 4), or jasmonic acid ([JA]; three; Table 4). In the more extensive cad2-1 specific group, a preliminary inspection of the annotation suggests that a high proportion of the affected genes may encode defense-related functions (see Supplemental Table 2S online). JA has been shown to influence glutathione metabolism by elevating transcript levels of -ECS, glutathione synthetase, and glutathione reductase (Xiang and Oliver, 1998). SA treatment of leaves leads to an increase in glutathione levels often ahead of induction of defense gene expression. This may influence the redox state of NPR1, a glutathione-sensitive regulatory protein in the SA signaling pathway in Arabidopsis (Mou et al., 2003). Confirmation of this observation comes from the increased growth of avirulent P. syringae in rax1-1 and cad2-1 plants, indicating that lowered glutathione levels are weakening these plants' defense capability (Figure 6). Thus, glutathione levels or its redox state does impact on stress defenses at the whole plant level.
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; Chang et al., 2004). In rax1-1, increased induction of APX2 expression over that of wild-type plants was observed in response to excess light and wounding (Figures 4 and 5B) and in cad2-1 after excess light stress (Figure 5B). Redox changes in photosynthetic electron transport and accumulation of H2O2 in vascular tissue have been identified as prerequisites for APX2 induction in wild-type plants (Karpinski et al., 1999; Fryer et al., 2003). However, neither in mesophyll nor vascular tissue of light stressed rax1-1 and cad2-1 plants were these parameters observed to differ from those of wild-type plants (see Supplemental Figure 3S online) nor was the pattern of change in glutathione levels different between mutants and the wild type subjected to excess light stress (data not shown). These data indicate that the mutants were no more affected by photooxidative stress at the whole plant level than Col-0; therefore, other signals must be the cause for enhanced APX2 expression. The expression of a further 12 stress-associated genes was skewed in excess light stressed mutants compared with the wild type (Figure 5B). These included six genes influenced by rax1-1 and cad2-1 under ambient conditions and six that were not. These data suggest that both the levels and biosynthesis of glutathione act in several different ways to influence stress defense mechanisms according to the physiological state of the plant.
Conclusion
Glutathione levels and its biosynthesis can profoundly affect the poising of stress defenses in plants, and this is achieved without any direct impact on cellular ROS levels. The direct interaction of glutathione or -ECS with one or more regulatory proteins may be how this control is achieved. In bacteria, yeast, animal, and plant cells, at least two mechanisms have been described by which glutathione can modulate the activity of signaling proteins independently of ROS levels. There are the so-called thiol switches, in which glutathione changes the redox state of thiol-groups of proteins that act as redox cofactors, altering either the activity or redox state of regulatory proteins, and secondly by S-glutathiolation of regulatory proteins with direct conjugation of glutathione to target Cys residues (Klatt and Lamas, 2000; Cooper et al., 2002; Delaunay et al., 2002; Mou et al., 2003; Paget and Buttner, 2003).
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METHODS |
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TOPABSTRACTINTRODUCTIONRESULTSDISCUSSIONMETHODSREFERENCES |
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). The APX2LUC transformant (Col-0) has been described previously (Karpinski et al., 1999). The 35S-GSH1 transgenic Arabidopsis line and cad2-1 were kind gifts from D.J. Oliver, Iowa State University, and C. Cobbett, University of Melbourne, Australia, respectively.
Plants were subjected to either complete or partial exposure to 5- to 15-fold excess light or wounding, as described previously (Karpinski et al., 1997, 1999; Chang et al., 2004). Vacuum infiltration of whole rosettes with avirulent Pseudomonas syringae pv tomato DC3000avrRpm1 was performed as described by Muskett et al. (2002).
Mutagenesis, Screening, and Mapping of rax1-1
APX2LUC seed were mutagenized in batches of 10,000 using 0.5% (v/v) ethyl methanesulfonate for 8 h. Ethyl methanesulfonate–treated seed had a germination frequency of 70%. Mutagenesis efficiency was confirmed in M1 plants by analyzing the frequency of chlorophyll deficiency in developing embryos from 100 siliques harvested from plants of each seed batch at 10 to 12 d postanthesis. M2 seeds were collected from independent pools of 500 M1 plants. M2 plants (500) from each pool were grown for 16 d under long day conditions, sprayed with 1 mM D (-)- luciferin (Karpinski et al., 1999), and assayed for their luciferase activity in 12-well microtitre dishes using a Victor Multilabel Counter 1420 workstation (Wallac, Finland). Plants were scored positive if one of the six readings was >100 cps (background was 30 to 40 cps). Positive plants (120) were repotted and grown for seed production. A repeat assay was done on 12 M3 progeny from each positive M2 rosette. Only phenotypically normal plants were kept to confirm the phenotype in the M3 generation. Inheritance of the phenotype was determined by following segregation after two subsequent backcrosses. The only two mutants from a total of 65 pools of M1 plants with a stably heritable, recessive phenotype were backcrossed to Col-0 a further three more times.
For the mapping of rax1, the strategy described by Jander et al. (2002) was adopted. DNA from 48 F2 progeny from a cross between the mutants and Arabidopsis Landsberg erecta that showed the luciferase positive, low glutathione phenotypes, were analyzed for the segregation of polymorphisms using custom-designed fluorescently tagged INDEL markers separated on an ABI 3700 capillary sequencer (Applied Biosystems, Foster City, CA). Identification of GSH1 on the map used information from TAIR (www.arabidopsis.org). Amplification and sequence determination of GSH1 and its full-length cDNA, from both versions of the rax1-1 mutation, was conducted using specific primers derived from the wild-type sequence. The John Innes Centre Genome Laboratory (www.jicgenomelab.co.uk) conducted both the sequencing and the mapping. The presence of both the rax1-1 and cad2-1 mutations in individual plants was confirmed by sequencing PCR products obtained with the following primer pair: 5'-ACCAACTATCTACGG-3' and 5'-CATACCAGAGTTATAAGGTGGG-3' (5' at 2572 and 3386 in EMBL accession number AF068299).
Imaging and Measurement of Luciferase Activity and H2O2 Accumulation
The imaging and in vitro determination of luciferase activity was as described previously (Karpinski et al., 1999; Chang et al., 2004). The visual detection of H2O2 was performed as described by Fryer et al. (2002). Total foliar H2O2 was determined as described by Creissen et al. (1999), except that 100 mg of Arabidopsis leaf tissue per 1 mL of extraction medium was used.
Preparation of RNA and RNA Gel Blots
Total RNA was isolated from leaves as described previously (Bechtold et al., 2004; Chang et al., 2004). A minimum of three RNA preparations each from a separate plant was made per time point. Preparation of RNA gel blots and the probes for APX1 (At1g07890.1), APX2 (At3g09640.1), and APX3 (At4g35000.1) have been described previously (Karpinski et al., 1997). Other probes used in the RNA gel blots or DNA gel blots were from ESTs obtained from the ABRC (Cleveland, OH). The inserts were amplified by PCR using universal and reverse primers. These ESTs used are as follows: APX4 (At1g77490.1, AA042529), APX5 (At4g08390.1, T41685), CAT1 (At1g70630.1, T43867), CAT2 (At4g35090, T41566), CAT3 (At1g20620.1, N38125), CSD1 (At1g08830.1, T42186), CSD2 (At2g28190.1, H36758), CSD3 (At5g18100.1, T88473), DHAR1 (At1g19570.1, H37392), DHAR2 (At1g75270, N37468), DHAR3 (At5g16710.1, H37601), FSD1 (At4g25100.2, AA042744), FSD2 (At5g51100.1, Y12641), GOR1 (At3g54660.1, D89620), GOR2 (At3g24170.1, U37697), GPX1 (At2g925080, AJ000469), GPX7 (At4g31875.1, NL049607), GSH1 (At4g23100.1, R84030), GSH2 (At5g27380.1, T43120), MDAR1 (At1g63940.2, T04550), MDAR2 (At5g03630.1, R64883), and MSD1 (At3g10920.1, T20828). The pea (Pisum sativum) ACTIN probe used to check RNA loadings was recovered by PCR from a full-length cDNA inserted the plasmid pBluescript SK+ (X67666) using T3 and T7 primers.
PCR Procedures for Analysis of RNA
The blotting and probing of 3'RACE products (Frohman et al., 1988) was used to analyze APX2 and APX1 expression as previously described (Bechtold et al., 2004; Chang et al., 2004). qRT-PCR was performed using a cybergreen fluorescence-based assay kit (DyNAmo SBYR Green qPCR kit; Finnzymes Oy, Espoo, Finland) according to the manufacturer's instructions. The PCR reactions and calculation were performed on an Opticon 2 real-time PCR machine using the manufacturer's software (Genetics Research Instrumentation, Braintree, UK). All mRNA levels were calculated from threshold cycle values and as relative to controls and normalized with respect to actin transcript levels according to Gruber et al. (2001). The primers used in qRT-PCR are given in Supplemental Table 2S online.
Microarray Analysis
Nine Affymetrix 8K GeneChips (Affymetrix, Santa Clara, CA; Zhu and Wang, 2000) were hybridized with target cRNA prepared from each of three independent RNA preparations for mutants and wild-type control. The plants were grown in a randomized block design mixing up plants for each of cad2-1, rax1-1, and the wild type (Col-0/APX2LUC). Each RNA preparation was pooled from eight 5-week-old short day–grown plants. RNA quality was assessed by running 1 µL of each RNA sample on Agilent RNA6000nano LabChips (Agilent Technology 2100 Bioanalyzer version A.01.20 SI211; Agilent Technologies, Palo Alto, CA). Affymetrix GeneChip array expression profiling was performed at the John Innes Centre Genome Lab, http://www.jicgenomelab.co.uk. All protocols used can be found in the Affymetrix Expression Analysis Technical Manual II (Affymetrix Manual II; http://www.affymetrix.com/support/technical/manuals.affx). After reading, the initial microarray data files were analyzed using Affymetrix software Microarray Suite (version 5.0). This included calculation of absolute values and normalization of the data with respect to internal standards. The data were then imported into Microsoft Excel, and three pairwise comparisons were performed of cad2-1 versus the wild type, rax1-1 versus the wild type, and a comparison of two randomly mixed samples. According to the detection call given to each probe set in each experiment (P, present; M, marginal; A, absent), the six data sets were classified and those having 6 P; 5 P + 1 M; 4 P + 2 M; 5 P + 1 A were accepted; all the others were discarded. The probe sets were sorted according to the differences in expression, and genes with less than a twofold difference were rejected. For each retained probe set, average signal in mutant, average signal in the wild type, fold change, and t test values were determined. The randomized test produced a list of 41 upregulated and four downregulated genes. The best t test values resulting from the randomized test were between 10 and 1000 times larger than those obtained in the mutant versus the wild type analyses. The identification of genes corresponding to the probe sets was performed using identifiers downloaded as a text file (affy8k-2002-12-23.txt) from the TAIR Web site (www.arabidopsis.org). Further analysis of the data used the following Web-based resources: The National Center for Biotechnology Information (http://www.ncbi.nlm.nih.gov/), The Institute for Genomic Research (www.tigr.org), the Affymetrix Web site, including Netaff-X tools (www.affymetrix.com), the Salk Institute Genomic Analysis Laboratory (http://signal.salk.edu/dgenome.html), and the Gene Ontology Consortium (www.geneontology.org/index.shtml).
Thiol Determinations
The determination of glutathione, -EC, and Cys contents as both oxidized and reduced forms was performed as previously described (Creissen et al., 1999; Bechtold et al., 2004).
Enzyme Assays
SOD, MDAR, and APX activity determinations were performed on Arabidopsis cell-free leaf extracts using the protocols of Jimenez et al. (1997). The activity of -ECS was determined in cell-free foliar extracts of Arabidopsis, prepared from 100 mg of leaf material per 1 mL of extraction buffer, essentially as described by Creissen et al. (1999). All data were calculated on a fresh weight basis.
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Acknowledgments |
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Footnotes |
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Online version contains Web-only data. 
Article, publication date, and citation information can be found at www.plantcell.org/cgi/doi/10.1105/tpc.104.022608.
Received March 15, 2004; accepted May 29, 2004.
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