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Loss-of-function of an Arabidopsis NADPH pyrophosphohydrolase, AtNUDX19, impacts on the pyridine nucleotides status and confers photooxidative stress tolerance

Scientific Reports volume 6, Article number: 37432 (2016) | Download Citation

Abstract

The levels and redox states of pyridine nucleotides, such as NADP(H), regulate the cellular redox homeostasis, which is crucial for photooxidative stress response in plants. However, how they are controlled is poorly understood. An Arabidopsis Nudix hydrolase, AtNUDX19, was previously identified to have NADPH hydrolytic activity in vitro, suggesting this enzyme to be a regulator of the NADPH status. We herein examined the physiological role of AtNUDX19 using its loss-of-function mutants. NADPH levels were increased in nudx19 mutants under both normal and high light conditions, while NADP+ and NAD+ levels were decreased. Despite the high redox states of NADP(H), nudx19 mutants exhibited high tolerance to moderate light- or methylviologen-induced photooxidative stresses. This tolerance might be partially attributed to the activation of either or both photosynthesis and the antioxidant system. Furthermore, a microarray analysis suggested the role of ANUDX19 in regulation of the salicylic acid (SA) response in a negative manner. Indeed, nudx19 mutants accumulated SA and showed high sensitivity to the hormone. Our findings demonstrate that ANUDX19 acts as an NADPH pyrophosphohydrolase to modulate cellular levels and redox states of pyridine nucleotides and fine-tunes photooxidative stress response through the regulation of photosynthesis, antioxidant system, and possibly hormonal signaling.

Introduction

The nicotinamide pyridine nucleotides, NAD(H) and its derivative NADP(H), play pivotal roles as redox compounds; they are ubiquitous co-factors that are required for hundreds of redox reactions in a number of metabolic pathways, including photosynthesis and the antioxidant system1. Pyridine nucleotides as well as reactive oxygen species (ROS) and antioxidants are therefore crucial determinants of cellular and organellar redox homeostasis, which modulate stress acclimation as well as growth and development in plants1,2,3.

In plant chloroplasts, the levels and redox states of NADP(H) are the determinant of ROS production by the photosynthetic transport chain (PET). The depletion of NADP+ as an electron acceptor, which often occurs under high light irradiation, excessively reduce PET, resulting in the facilitation of oxygen reduction followed by ROS production (photooxidative stress)4,5. Plants have evolved a number of mechanisms, including antioxidant systems and light energy dissipation as heat (xanthophyll cycle), thereby avoiding or acclimating to the oxidative stress caused by illumination4,5,6,7. NADPH also serves as the source of reducing equivalents for the ascorbate-glutathione cycle and the thioredoxin-dependent network, two major antioxidant systems in plant cells2, and also for the xanthophyll cycle, because this requires ascorbate, which is recycled using ferredoxin or NADPH. Thus, the redox states of NADP(H) are crucial for regulating both ROS production and scavenging in chloroplasts.

Pyridine nucleotides have also been characterized as signals that regulate stress and hormonal responses in plants. In Arabidopsis leaves, treatments with NAD+, NADH, NADP+, and NADPH enhanced the levels of salicylic acid (SA), a phytohormone essential for the biotic stress response, and the expression of PATHOGENESIS-RELATED1 (PR1)8, a representative SA-responsive gene. Since the plasma membrane is highly impermeable to pyridine nucleotides1, these findings indicate that extracellular pyridine nucleotides act as signals to induce the SA-dependent biotic stress response. Pétriacq et al.9 recently created transgenic Arabidopsis plants that overexpressed a bacterial quinolinate phosphoribosyltransferase gene. In the transgenic plants, a quinolinate treatment increased the intracellular levels of all pyridine nucleotides, especially NAD+, resulting in enhanced SA levels and PR1 expression. Thus, both intracellular and extracellular pyridine nucleotides positively regulate the SA pathway. Pyridine nucleotides also serve as the precursors for cyclic ADP-ribose and nicotinic acid adenine dinucleotide phosphate, intracellular Ca2+-mobilizing agents, which promotes the release of Ca2+ from stores10. In addition to their function in the cellular redox homeostasis, these facts indicate that the levels and redox states of pyridine nucleotides must be tightly controlled to fine-tune plant responses to stress and hormone.

A number of metabolic pathways, including primary metabolisms and synthesis of pyridine nucleotides, are involved in the regulation of pyridine nucleotides levels and redox states. The pyridine nucleotide synthesis and its role in photooxidative stress response have been addressed. For example, Arabidopsis NAD kinase 2 (AtNADK2), which catalyzes the phosphorylation of NAD+ to produce NADP+ in chloroplasts, has been shown to be essential for normal growth, photosynthesis, and photooxidative stress tolerance11,12. However, the mode of action of pyridine nucleotide catabolism and its physiological role are poorly understood. One of candidates involved in the catabolic process is Nudix (nucleoside diphosphates linked to some moiety X) hydrolase family, having hydrolytic activity toward various nucleoside diphosphate derivatives, which include NADH and NADPH, and being widely distributed among all classes of organisms13,14,15,16. Arabidopsis possesses 28 Nudix hydrolases (AtNUDXs) and some isoforms that have NADH hydrolase activity, such as AtNUDX6 and AtNUDX7, though the latter also uses ADP-ribose as an alternative substrate17. AtNUDX6 and 7 are known to act as positive and negative regulators, respectively, of SA-induced gene expression18,19,20,21,22,23. This provides further evidence that the regulation of cellular NADH levels through Nudix enzymes is critical for SA-mediated responses.

Among the different AtNUDXs, AtNUDX19 (At5g20070), which is known to be targeted to both chloroplasts and peroxisomes24,25, is currently the only enzyme to exhibit pyrophosphohydrolase activity toward NADPH in vitro24, suggesting that this enzyme participates in plant response to photooxidative stress by regulating the NADPH levels. Indeed, AtNUDX19 was very recently found to regulate NADPH levels and activity of enzymes involved in the NADPH production in Arabidopsis leaves and roots26. We herein examined the physiological roles of AtNUDX19 and found that this enzyme is a new regulator of the levels and redox states of pyridine nucleotides and fine-tunes the photooxidative stress response in plant cells.

Results

Structure and distribution of AtNUDX19 type enzymes in plants

Compared to other Nudix isoforms, AtNUDX19 and its homologues have been poorly characterized in plants. Therefore, we started with analyses of structure, distribution, and evolutional history of this new enzyme. Using the Pfam database (version 29.0)27, we found that AtNUDX19 consists of three domains; i.e., NADH pyrophosphatase-like rudimentary NUDIX domain (NUDIX-like, PF09296), NADH pyrophosphatase zinc ribbon domain (zf-NADH-PPase: PF09297), and NUDIX domain (PF00293) (Fig. 1a). An obvious Nudix motif (GX5EX7REUXEEXGU)16 was observed in the NUDIX domain (Supplemental Figure S1), but not in the NUDIX-like, probably suggesting the later domain to have no hydrolase activity. The zf-NADH-PPase domain was located between the NUDIX-like and NUDIX domains. AtNUDX19 is known to have the SQPWPFPxS motif 28 immediately downstream of the Nudix motif within the NUDIX domain (see Supplemental Figure S1). According to previous classification of Arabidopsis isoforms29, only AtNUDX19 belongs to the NADH pyrophosphohydrolase group. However, the group name ‘NADH pyrophosphohydrolase’ is inadequate to explain the function of AtNUDX19 owing to the following reasons; (1) other isoforms in the FGFTNE (fibroblast growth factor) group, such as AtNUDX6 and 7, also have NADH pyrophosphohydrolase activity17, and (2) AtNUDX19 has little activity toward NADH in vivo (see the following results and discussion). Therefore, we refer this as the ‘SQPWP’ group in this study because of the presence of the SQPWPFPxS motif, which is lacked in isoforms of other groups29.

Figure 1: Structure and phylogenetic tree of AtNUDX19-type (SQPWP) enzymes.
Figure 1

(a) Structure of subgroup I (AtNUDX19) and II (Klebsormidium flaccidum, kfl00032_0450) enzymes. (b) SQPWP sequences from various photosynthetic eukaryotes, which are Arabidopsis thaliana (AtNUDX19), Triticum aestivum L. (TaNUDT1), Eucalyptus grandis, Manihot esculenta, Populus trichocarpa, Solanum lycopersicum, Amborella trichopoda, Sorghum bicolor, Brachypodium distachyon, Oryza sativa, Physcomitrella patens, Klebsormidium flaccidum, Volvox carteri, Chlamydomonas reinhardtii, Coccomyxa subellipsoidea C-169, Micromonas pusilla CCMP1545, and Micromonas sp. RCC299. Accession numbers for these sequences are available in Supplemental Table S1. The phylogenetic tree was generated by the neighbor-joining method with 1,000 bootstraps using MEGA7 software.

We then examined the sequenced genomes of various plant species, including algae, moss, and higher plants, for the presence of the SQPWP enzyme(s). All photosynthetic eukaryotes analyzed possessed more than one isoform (Supplemental Table S1), while no photosynthetic prokaryotes with this group was found (using Cyanobase)30; only one exception was Rhodopseudomonas palustris CGA009, photosynthetic bacteria, which had the SQPWP enzyme (RPA0613, data not shown). Like AtNUDX19, these enzymes had the NUDIX, NUDIX-like, and zf-NADH-PPase domains and the Nudix and SQPWPFPxS motifs with some exceptions (see Supplemental Table S1). Thus, the SQPWP group is widely distributed in photosynthetic eukaryotes, although it remains to be experimentally addressed whether these can use pyridine nucleotides as substrates. Phylogenetic analysis revealed that their sequences could be divided into further 2 subgroups (I and II) (Fig. 1b). Higher plants contained only subgroup I, while moss (Physcomitrella patens), the charophyte (Klebsormidium flaccidum), and the chlorophytes (Chlamydomonas reinhardtii and Volvox carteri) had both subgroups. In contrast, the trebouxiophyte (Coccomyxa subellipsoidea C-169, also known as Chlorella vulgaris) and the prasinophytes (Micromonas pusilla CCMP1545 and Micromonas sp. RCC299) possessed only subgroup II. These findings suggest that subgroup II was ancestral and then lost in higher plants, which have another subgroup I acquired in the chlorophytes. All enzymes in subgroup II, except for the Micromonas enzymes, had an additional Oncus domain (Supplemental Table S1), which was found in the testes-specific Janus/Ocnus family proteins in Drosophila melanogaster31. Almost subgroup I enzymes possessed both chloroplast- and peroxisome-targeting signals (Supplemental Table S2). Indeed, AtNUDX19 was experimentally confirmed to be localized in both organelles24,25.

The levels and redox states of Pyridine nucleotides in nudx19 mutants

To investigate the physiological function of AtNUDX19, Arabidopsis lines (SALK_115339 and SALK_135053) containing a T-DNA insert in the AtNUDX19 gene were used in this study. Both lines contained a T-DNA in the fourth intron region of the gene (Supplemental Figure S2). As described in Corpas et al.26, neither transcript nor protein of AtNUDX19 was detected in the homozygous SALK_135053 line (Supplemental Figure S2). In contrast, very low levels of the AtNUDX19 transcript and protein were observed in the homozygous SALK_115339 line. Thus, the SALK_135053 and SALK_115339 lines were knockout (KO-nudx19) and knockdown (KD-nudx19) mutants of this gene, respectively. The growth of these mutants was similar to that of wild-type plants under normal growth conditions (16 h of 100 μmol photons m−2 s−1, 8 h of dark).

We then investigated the effects of disrupting AtNUDX19 on pyridine nucleotides levels in leaves. Three-week-old wild type and nudx19 mutants grown under normal light conditions were exposed to high light (1,200 μmol photons m−2 s−1) for 6 h. Under both normal and high light intensities, NADPH levels were significantly higher in both KD- and KO-nudx19 plants than in the wild-type plants (Fig. 2). Interestingly, NADP+ levels were lower in KD- and KO-nudx19 plants under normal light, but recovered to the wild-type levels by high light exposure. As a consequent, total NADP(H) levels in the nudx19 mutants were lower than those in the wild-type plants under normal light, but slightly higher after high light exposure (Table 1). The ratio of NADPH to total NADP(H) in KD- and KO-nudx19 plants was approximately 2-fold higher than that in wild type under both conditions. The lack of AtNUDX19 had no impact on NADH levels (Fig. 2). Under normal light intensity, there was also no difference in NAD+ levels between wild-type and mutant plants. Although NAD+ levels were increased in response to high light in wild type, this increase was almost completely inhibited in the nudx19 mutants (Fig. 2), which increased the ratio of NADH to total NAD(H) (Table 1). Together with its enzymological properties obtained from in vitro assay24, current findings demonstrate that AtNUDX19 catalyzes the hydrolysis of NADPH, but not NADH, in vivo and has significant impacts on the cellular levels and redox states of pyridine nucleotides.

Figure 2: Pyridine nucleotides levels in wild-type and nudx19 mutants.
Figure 2

Three-week-old wild-type (WT) and mutant plants (KD and KO) were exposed to high light (1,000 μmol photons m−2 s−1) for 6 h. The levels of pyridine nucleotides, NADPH (a), NADH (b), NADP+ (c), and NAD+ (d), in leaves were measured. Data are means ± SD for at least 3 individual experiments (≥5 plants for 1 experiment). Significant differences: *P < 0.05 vs. the value of wild-type plants.

Table 1: Levels and redox states of pyridine nucleotides in nudx19 mutants.

We also checked the effect of light intensity on the AtNUDX19 expression. When 1-week-old wild-type plants were further grown under different light intensities (16 h of 20, 100, and 800 μmol photons m−2 s−1, 8 h of dark) for 2 weeks, the increase in the intensity of growth light had positive effect on the transcript levels of AtNUDX19 but not on its protein levels (Supplemental Figure S3).

Photooxidative stress tolerance of nudx19 mutants

Before and after high light exposure, nudx19 mutants showed high reduction state of NADPH (Table 1), which, in general, can excessive reduce PET, thereby enhancing ROS production4. Although we did not address whether the redox change occurred within chloroplasts, our findings implied that nudx19 might be highly sensitive to photooxidative stress. However, when 1-week-old wild-type and nudx19 plants were grown further under moderate light conditions (16 h of 450 μmol photons m−2 s−1, 8 h of dark) for 2 weeks, the growth of KO- and KD-nudx19 plants was unexpectedly but clearly enhanced (Fig. 3a). Furthermore, KO- and KD-nudx19 plants were highly tolerant to the treatment with methylviologen (MV), a ROS-producing agent in chloroplasts and mitochondria (Fig. 3b,c), suggesting the nudx19 mutants to be insensitive to oxidative stress.

Figure 3: Tolerance of nudx19 mutants to photooxidative stress.
Figure 3

(a) One-week-old wild-type and mutants, grown on MS medium under normal light conditions, were transferred to soil and grown further under moderate light stress conditions (16 h of 400 μmol photons m−2 s−1, and 8 h of dark). Photograph of seedlings 2 weeks after transferring to moderate light conditions. The same results were obtained in 4 independent experiments. The results of the representative leaves were photographed. (b,c) Ten-day-old wild-type and mutants, grown on MS medium under normal light conditions, were transferred to medium containing 4 μM methylviologen (MV), an ROS generator, and grown further for 1 week under the same light conditions. (b) Photograph of seedlings 1 week after the MV treatment. The same results were obtained in 4 independent experiments. The results of representative leaves were photographed. (c) Chlorophyll contents in shoots. Data are means ± SD for 4 individual experiments (≥10 plants for 1 experiment). Significant differences: *P < 0.05 vs. the value of wild-type plants.

Photosynthesis in nudx19 mutants under high light

We hypothesized that the tolerance of nudx19 mutants to photooxidative stress was due to an enhancement in photosynthesis, increase in antioxidant capacity, and/or modulation of the expression of defense genes through changes in the levels and redox states of NAD(P)(H). To clarify the effects of disrupting AtNUDX19 on PET, the quantum yield of photosystem II (øPSII) and photochemical and nonphotochemical quenching (qP and NPQ, respectively) were measured under high light in wild-type and nudx19 plants (Fig. 4). 1-qP indicates the reduction states of PSII32. In all genotypes, 1-qP and NPQ were increased by high light irradiation (6 h), whereas øPSII was decreased. However, the increase in 1-qP was mitigated in KO- and KD-nudx19 plants, although the lack of AtNUDX19 had no significant effect on NPQ (Fig. 4). The decrease in øPSII was also suppressed in KO- and KD-nudx19 plants (Fig. 4). These results indicate that nudx19 mutants could prevent the excessive reduction of PET more than wild-type plants.

Figure 4: Photosynthetic parameters in nudx19 mutants under high light.
Figure 4

Three-week-old wild-type and mutant plants were exposed to high light (1,000 μmol photons m−2 s−1). (a–c) øPSII, 1-qP, and NPQ in leaves was determined at 25 °C after dark adaptation for 15 min. Data are means ± SD for 4 individual experiments. (d, e) The initial activities of FBPase and SBPase in leaves were measured. Data are means ± SD for 4 individual experiments (≥3 plants for 1 experiment). Significant differences: *P < 0.05 vs. the value of wild-type plants. (f) CO2 fixation was measured in leaves with an LI-6400 portable photosynthesis system. Each data point represents the mean ± SD of at least 5 individual experiments.

We also examined the activities of enzymes involved in the Calvin cycle, sedoheptulose-1,7-bisphosphatase (SBPase) and fructose-1,6-bisphosphatase (FBPase), which are tightly controlled through thiol-dependent redox regulation. Although the lack of AtNUDX19 had no effect on the total activities of SBPase and FBPase under normal and high light conditions (data not shown), the initial activities of these enzymes were significantly higher in nudx19 mutants than in wild-type plants during high light exposure (Fig. 4). In line with this, the carbon assimilation rate was also higher in nudx19 mutants than in wild-type plants above a light intensity of 200 μmol photons m−2 s−1, especially at a saturating irradiance (1,200 μmol photons m−2 s−1).

Activity of antioxidant enzymes in nudx19 mutants

We then measured the total activities of antioxidative enzymes, ascorbate peroxidase (APX), dehydroascorbate reductase (DHAR), monodehydroascorbate reductase (MDAR), and glutathione reductase (GR), all of which are components of the ascorbate-glutathione cycle, one of the main systems for scavenging ROS in plant cells2,3,4. Before high light exposure, no significant difference was observed in the activities of any of these enzymes between wild-type and nudx19 plants (Fig. 5). However, all the activities, except for GR, were slightly but significantly higher in KO- and KD-nudx19 plants than in wild-type plants after 6 h of high light exposure (Fig. 5). These results suggest that the disruption of AtNUDX19 activates both photosynthetic and antioxidative capacities under high light, possibly leading to higher tolerance to the stress.

Figure 5: Activities of antioxidative enzymes in nudx19 mutants under high light.
Figure 5

Three-week-old wild-type and mutant plants were exposed to high light (1,000 μmol photons m−2 s−1) for 6 h. The activities of APX (a), GR (b), DHAR (c), and MDAR (d) in leaves were measured. Data are means ±SD for 4 individual experiments (≥3 plants for 1 experiment). Significant differences: *P < 0.05 vs. the value of wild-type plants.

Effects of AtNUDX19-disruption on nuclear gene expression

A microarray analysis was performed using wild-type and KO-nudx19 leaves under normal growth conditions to investigate the effects of the altered NADPH status on gene expression. Differences in the change ratio of gene expression were evaluated by the Wilcoxon signed-rank test and multiple testing problems were corrected by the Benjamini-Hochberg method33. Genes with expression levels that were 1.5-fold higher (37 genes) or lower (16 genes) in KO-nudx19 leaves than in wild-type leaves were selected (Supplemental Table S2). No gene encoding antioxidative enzyme, such as APX, DHAR, MDAR, and GR, was included in the up-regulated genes. Furthermore, only one gene among the up-regulated genes, light harvesting complex 1 (LHCA1), encoded a photosynthesis-related gene.

We found 2 representative SA-responsive genes, PR1 and PR2, among the up-regulated genes (Supplemental Table S2). In addition, the transcript levels of SYSTEMYC AQUIRED RESISTANCE DEDICIENT1 (SARD1) and the WRKY38 transcription factors, which are known to be involved in the SA-dependent pathogen response20,34,35, were enhanced in KO-nudx19 leaves (Supplemental Table S2). Notably, SARD1 binds to the promoter of SALICYLIC ACID INDUCTION DEFICIE2 (SID2) gene encoding an isochorismate synthase, which is required for SA biosynthesis in Arabidopsis, and activates its expression35. Therefore, we investigated the effects of nudx19 mutations on the levels of and sensitivity to SA. The levels of free SA were significantly enhanced in nudx19 mutants under normal and high light (Fig. 6a). Furthermore, when 3-day-old plants were grown on MS medium containing SA (25 and 50 μM) for a further 5 days, KO- and KD-nudx19 plants were slightly but significantly more sensitive to the treatment than wild-type plants (Fig. 6b). We also found that the expression of AtNUDX19 was responsive to the SA treatment (Supplemental Figure S4). These results indicate that AtNUDX19 acts as a negative regulator of SA synthesis. In contrast, KO- and KD-nudx19 plants were slightly insensitive to jasmonic acid methyl (MeJA) and abscisic acid (ABA) (Fig. 6b). This might be explained by the fact that SA acts as an antagonist of these hormones36,37. The expression of AtNUDX19 was also responsive to treatments with these hormones (Supplemental Figure S4).

Figure 6: Effect of nudx19 mutations on SA levels and sensitivity to hormones.
Figure 6

(a) Three-week-old wild-type and mutant plants were exposed to high light (1,000 μmol photons m−2 s−1) for 6 h. Free SA levels in leaves were measured. Data are means ± SD for 6 individual experiments (≥5 plants for 1 experiment). (b) Three-day-old wild-type and mutant plants, grown on MS medium, were transferred to and further grown on medium containing SA (25 and 50 μM), MeJA (12.5 and 25 μM), and ABA (10 and 20 μM). Root length was measured 5 days after the treatment. Data are means ± SD for at least 3 individual experiments (≥10 seedlings for 1 experiment). Significant differences: *P < 0.05 vs. the value of wild-type plants.

Discussion

Here, we addressed the physiological function of AtNUDX19, which is widely distributed throughout photosynthetic eukaryotes (Fig. 1), in photooxidative stress response using its loss-of-function mutants. Our findings indicate that 1) only NADPH is a physiological substrate of the enzyme in vivo, (2) AtNUDX19 regulates cellular levels and redox states of pyridine nucleotides, and (3) this regulation is associated with plant responses to photooxidative stress and hormones.

Our previous in vitro assay showed that a recombinant AtNUDX19 protein can hydrolyze both NADPH and NADH, but its Km value for NADPH (36.9 μM) is approximately 9-fold lower than that for NADH (335.3 μM), suggesting that AtNUDX19 prefers NADPH to NADH as a substrate24. Similarly, a wheat Nudix hydrolase (TaNUDT1) strongly prefers NADPH38. In line with these findings, the present study showed that the levels of NADPH, but not other pyridine nucleotides, were enhanced in AtNUDX19-disrupted mutants (Fig. 2). These results strongly indicate AtNUDX19 to hydrolyze NADPH, but not NADH, in vivo. As described above, AtNUDX19 is targeted to both chloroplasts and peroxisomes24,25. In chloroplast stroma, the concentration of NADPH has been estimated to be 0.29 to 0.5 mM in light and 0.12 mM in darkness39,40, whereas that in peroxisomes is presently unknown. Furthermore, 60–85% of total cellular NADPH is present in illuminated chloroplasts41. Thus, the chloroplastic localization of AtNUDX19 is likely to be suitable for its enzymatic reaction.

The lack of AtNUDX19 had significant impacts on the levels and redox states of pyridine nucleotides (Fig. 2). For example, levels of NADP+ were lower in the mutants than in wild type, resulting in a decrease in total NADP(H) under normal light. It is currently difficult to provide an exact explanation how AtNUDX19 affects the pyridine nucleotides status in plant cells, because their redox states are finely tuned through various metabolic pathways. One of possible explanations might be provided by a recent finding that the lack of AtNUDX19 stimulated the activity of enzymes involved in the NADPH production from NADP+; i.e., NADP-isocitrate dehydrogenase, NADP-malicenzyme, glucose-6-phosphate dehydrogenase and 6-phosphogluconate dehydrogenase26. These enzymes might be activated to produce more NADPH in nudx19 mutants, which resulted in the decrease of NADP+.

One of unexpected results was that despite a high NADPH/NADP+ ratio, nudx19 mutants were highly tolerant to photooxidative stresses (Figs 2 and 3 and Table 1). The measurement of chlorophyll fluorescence indicated that the nudx19 mutations could prevent the excessive reduction of PET (Fig. 4). This might be partially due to the activation of photosynthetic carbon assimilation and antioxidant systems in the nudx19 mutants (Figs 4 and 5), because these pathways can act as electron sink for PET4. Although how these systems were activated in nudx19 mutants is currently unknown, NADPH is known to function as a positive effector to promote the activation of ribulose 1,5-bisphosphate carboxylase/oxygenase (Rubisco), a key enzyme of the Calvin cycle42,43. The activation of photosynthesis was also observed in transgenic Arabidopsis and rice lines overexpressing chloroplastic NADK244,45. Unlike NADK2-overexpressing plants, in which the levels of both NADP+ and NADPH were increased44,45, the nudx19 mutants only accumulated NADPH and no other pyridine nucleotides (Fig. 2). Assuming that photosynthesis is enhanced through the same mechanism in both nudx19 mutants and NADK2-overexpressors, these findings suggest that NADPH is more critical for the enhancement of photosynthesis than NADP+.

A microarray analysis revealed that expression of approximately 50 genes was affected in nudx19 mutants (Supplemental Table S2), allowing us to expect that these changes might also be associated with the photooxidative stress tolerance of the mutants. Interestingly, two of up-regulated genes were PR1 and PR2, which was in line with the elevated levels of SA and high sensitivity to the hormone (Fig. 6). As described above, intracellular and extracellular pyridine nucleotides can activate the SA pathway irrespective of the kinds of pyridine nucleotides8,9. These observations indicate that the enhanced NADPH levels in these mutants activate SA biosynthesis, and that AtNUDX19 acts as a negative regulator of SA biosynthesis and its response. Since controlled levels of SA were also previously shown to be required for optimal photosynthesis46, the enhanced SA pathway might affect the abilities of photosynthesis and antioxidant defense in nudx19 mutants. In agreement with previous findings that SA is an antagonist of JA and ABA36,37, nudx19 mutants showed an insensitivity to MeJA and ABA (Fig. 6), although it should be experimentally investigated if the insensitivity was due to the activation of the SA pathway.

Taken together, our results demonstrate that AtNUDX19 is a novel regulator of the pyridine nucleotides status to modulate plant response to photooxidative stress and hormones, although more studies are required to elucidate the mechanism(s) underlying how the pyridine nucleotides status modulate such responses. Since other Nudix hydrolases having NADH (but not NADPH) hydrolytic activity, such as AtNUDX6 and 7, are also involved in the photooxidative response in a positive manner, it will also be interesting to investigate the crosstalk between these AtNUDX isoforms and AtNUDX19 in the fine-tuning of stress and hormonal responses in future studies.

Methods

Plant materials and growth conditions

Arabidopsis thaliana (Col-0) was used as wild type in this study. Two T-DNA insertion lines for AtNUDX19 gene (SALK_135053 and SALK_115339) were obtained from Arabidopsis Biological Resource Centre. To achieve normal growth, surface-sterilized seeds were sown on Murashige and Skoog (MS) medium containing 3% sucrose. Plates were stratified in darkness for 2 or 3 days at 4 °C and then transferred to a growth chamber kept at 23 °C during 16 h of light (100 μmol photons m−2 s−1) and at 22 °C during 8 h of darkness. After 7 days, seedlings were potted in soil and grown under the same conditions. The methods used for the applications of stresses and hormones are described in the figure legends.

Preparation of total RNA, cDNA synthesis, and semi-quantitative RT-PCR analysis

Total RNA was isolated from the leaves of Arabidopsis plants using Sepasol-RNA I (Nacalai Tesque, Kyoto, Japan). First strand cDNA was synthesized using reverse transcriptase (ReverTra Ace; Toyobo) with an oligo dT primer. These analyses were performed according to the manufacturer’s instructions. A semi-quantitative RT-PCR analysis was performed according to Ogawa et al.17. Primer sequences are as follows; AtNUDX19-F (5′-ATGCTTGCTCTCTTCCTCTC-3′), AtNUDX19-R (5′-CTACAAACTTGAGAGAGAGACACC-3′), Actin8-F (5′-GAGATCCACATCTGCTGG-3′), and Actin8-R (5′-GCTGAGAGATTCAGGTGCCC-3′).

Quantitative RT-PCR (q-PCR) analysis

Primer pairs for q-PCR were designed using PRIMER EXPRESS software (Applied Biosystems). Primer sequences are as follows; AtNUDX19-QF (5′-TTTGGCAGAGGATGGTTTCG-3′), AtNUDX19-QR (5′-GCCAACTCATCCATAGCACGTT-3′), Actin2-QF (5′-GGTGGTTCCATTCTTGCTTCCC-3′), Actin2-QR (5′-TCATACTCGGCCTTGGAGATCC-3′). Gene-specific primers were chosen such that the resulting PCR product had an approximately equal size of 100 bp. q-PCR was performed with an Applied Biosystems 7300 Real Time PCR System, using the SYBR Premix Ex Taq (Takara). Actin2 mRNA was used as an internal standard in all experiments.

Western blotting

The Western blot analysis was carried out as described previously24. The protein bands were detected using a polyclonal rabbit antibody (anti-AtNUDX19) prepared using the recombinant protein as the primary antibody and anti-rabbit IgG-HRP conjugate (Bio-Rad, CA) as the secondary antibody.

Measurements of pyridine nucleotides and free SA

NAD+, NADH, NADP+, and NADPH levels were measured according to Ishikawa et al.20. Free SA levels were measured according to Maruta et al.47.

Measurements of chlorophyll fluorescence and carbon assimilation rates

Chlorophyll fluorescence in Arabidopsis leaves was measured after dark adaptation for 20 min at 23 °C with a Junior-PAM (Waltz, Efeltrich, Germany). The actinic irradiance used was 120 (for normal light) or 400 μmol photons m−2 s−1 (for high light). The quenching parameters, qP and NPQ, were calculated according to van Kooten & Snel48.

Enzyme assays

The soluble fraction extracted from 0.2 g of Arabidopsis leaves was used for all enzyme assays. APX activity was measured as a decrease in absorbance at 290 nm (ε = 2.8 mM cm−1) due to the oxidation of ascorbate. Leaves were homogenized with 400 μl of 50 mM potassium phosphate (pH 7.5) containing 1 mM EDTA and 10% D-solbitol for the DHAR and GR assays, while leaves were homogenized with 400 μl of 50 mM potassium phosphate (pH 7.5) containing 0.2 mM EDTA, 10 mM 2-mercaptoethanol, and 1% D-solbitol for the MDAR assay. After centrifugation (20,000 × g) for 20 min at 4 °C, the supernatant obtained was used for these enzyme assays. In the DHAR assay, 20 μl of extract was added to 1 ml of reaction mixture containing 50 mM potassium phosphate (pH 7.5), 2 mM GSH, and 1 mM DHA, 0.2 mM NADPH, and GR. glutathione-dependent dehydroascorbate reduction was monitored at 340 nm. In the MDAR assay, 20 μl of extract was added to 1 ml of reaction mixture containing 100 mM potassium phosphate (pH 7.5), 1 mM ascorbate, and 0.2 mM NADPH. The reaction was started by the addition of 0.2 unit ascorbate oxidase after pre-incubation for 2 min. NADPH-dependent MDAR activity was monitored at 340 nm. In the GR assay, 10 μl of extract was added to 1 ml of reaction mixture containing 100 mM Tris-HCl (pH 7.8), 0.5 mM oxidized glutathione, 0.05 mM NADPH, and 0.5 mM EDTA. The reaction was started by the addition of NADPH and GSSG-dependent NADPH oxidation was monitored at 340 nm.

To measure the initial activities of SBPase and FBPase, leaf tissues were homogenized with 400 μl of 100 mM Tris–HCl buffer (pH 8.0), 16 mM MgCl2, 1 mM EDTA, 2% (w/v) PVP, and 0.05% Triton X-100. The maximum activities of both enzymes were determined by preincubating crude extracts with 20 mM dithiothreitol (DTT). The activities of both enzymes were measured according to Tamoi et al.49.

Microarray and data analyses

The quality and purity of RNA were confirmed for the microarray analysis with an Ultrospec 2100 pro (GE Healthcare UK Ltd). Total RNA samples were reverse-transcribed, yielding double-strand cDNA, which was transcribed in vitro in the presence of biotin-labeled nucleotides with an IVT Labeling Kit (Affymetrix Inc.), and purified. Labeled cRNA was fragmented and hybridized to Affymetrix ATH1 GeneChip arrays for 16 h at 45 °C according to Affymetrix protocols. Arrays were washed on an Affymetrix Fluidics Station 450 and measured for fluorescence intensity with an Affymetrix GeneChip Scanner 3000. Raw data were processed using Affymetrix Gene Chip Operating Software (GCOS; Version 1.4.0.036). Two biological replicates were analyzed. We initially calculated the log2 (ratio) of gene expression and P-values based on the one-sided Wilcoxon signed-rank test for nudx19 mutants against Col-0 by GCOS. Q values (adjusted P-values) were calculated from P-values by the Benjamini-Hochberg method33. In this experiment, we excluded 64 controls and 2,191 genes subject to cross-hybridization, according to NetAffx Annotation (www.affymetrix.com). We finally selected 37 up-regulated genes and 16 down-regulated genes, these genes showed >1.5-fold and q < 0.20 commonly for both replication sets. The criteria of q < 0.20 is often used for corrections of multiple testing problems50.

Additional Information

Accession codes: The microarray data were deposited in the public NCBI Gene Expression Omnibus database under the GEO accession number GSE64968.

How to cite this article: Maruta, T. et al. Loss-of-function of an Arabidopsis NADPH pyrophosphohydrolase, AtNUDX19, impacts on the pyridine nucleotides status and confers photooxidative stress tolerance. Sci. Rep. 6, 37432; doi: 10.1038/srep37432 (2016).

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References

  1. 1.

    et al. NAD(P) synthesis and pyridine nucleotide cycling in plants and their potential importance in stress conditions. J. Exp. Bot. 57, 1603–1620 (2006).

  2. 2.

    & Understanding oxidative stress and antioxidant functions to enhance photosynthesis. Plant Physiol. 155, 93–100 (2011).

  3. 3.

    & Cellular redox regulation, signaling, and stress response in plants. Biosci. Biotechnol. Biochem. 78, 1457–1470 (2014).

  4. 4.

    The Water-Water Cycle in Chloroplasts: Scavenging of Active Oxygens and Dissipation of Excess Photons. Annu. Rev. Plant Physiol. Plant Mol. Biol. 50, 601–639 (1999).

  5. 5.

    et al. Diversity and Evolution of Ascorbate Peroxidase Functions in Chloroplasts: More Than Just a Classical Antioxidant Enzyme? Plant Cell Physiol. 57, 1377–1386 (2016).

  6. 6.

    1999. Photoprotection Revisited: Genetic and Molecular Approaches. Annu. Rev. Plant Physiol. Plant Mol. Biol. 50, 333–359 (1999).

  7. 7.

    Central role of cyclic electron transport around photosystem I in the regulation of photosynthesis. Curr. Opin. Biotechnol. 26, 25–30 (2014).

  8. 8.

    & Extracellular pyridine nucleotides induce PR gene expression and disease resistance in Arabidopsis. Plant J. 57, 302–312 (2009).

  9. 9.

    et al. Inducible NAD overproduction in Arabidopsis alters metabolic pools and gene expression correlated with increased salicylate content and resistance to Pst-AvrRpm1. Plant J. 70, 650–665 (2012).

  10. 10.

    et al. NAD-new roles in signalling and gene regulation in plants. New Phytol. 163, 31–44 (2004).

  11. 11.

    et al. NADK2, an Arabidopsis chloroplastic NAD kinase, plays a vital role in both chlorophyll synthesis and chloroplast protection. Plant Mol. Biol. 59, 553–564 (2005).

  12. 12.

    et al. Chloroplast NAD kinase is essential for energy transduction through the xanthophyll cycle in photosynthesis. Plant Cell Physiol. 47, 1678–1682 (2006).

  13. 13.

    et al. The MutT proteins or “Nudix” hydrolases, a family of versatile, widely distributed, “housecleaning” enzymes. J. Biol. Chem. 271, 25059–25062 (1996).

  14. 14.

    et al. The 26 Nudix hydrolases of Bacillus cereus, a close relative of Bacillus anthracis. J. Biol. Chem. 279, 24861–24865 (2004).

  15. 15.

    The plant Nudix hydrolase family. Acta Biochim. Pol. 55, 663–671 (2008).

  16. 16.

    & Versatile physiological functions of the Nudix hydrolase family in Arabidopsis. Biosci. Biotechnol. Biochem. 79, 1–13 (2015).

  17. 17.

    et al. Comprehensive analysis of cytosolic Nudix hydrolases in Arabidopsis thaliana. J. Biol. Chem. 280, 25277–25283 (2005).

  18. 18.

    et al. Salicylic acid-independent enhanced disease susceptibility1 signaling in Arabidopsis immunity and cell death is regulated by the monooxygenase FMO1 and the Nudix hydrolase NUDT7. Plant Cell 18, 1038–1051 (2006).

  19. 19.

    et al. AtNUDT7, a negative regulator of basal immunity in Arabidopsis, modulates two distinct defense response pathways and is involved in maintaining redox homeostasis. Plant Physiol. 145, 204–215 (2007).

  20. 20.

    et al. AtNUDX6, an ADP-ribose/NADH pyrophosphohydrolase in Arabidopsis, positively regulates NPR1-dependent salicylic acid signaling. Plant Physiol. 152, 2000–2012 (2010).

  21. 21.

    et al. Salicylic acid antagonism of EDS1-driven cell death is important for immune and oxidative stress responses in Arabidopsis. Plant J. 62, 628–640 (2010).

  22. 22.

    et al. The ammonium/nitrate ratio is an input signal in the temperature-modulated, SNC1-mediated and EDS1-dependent autoimmunity of nudt6-2 nudt7. Plant J. 73, 262–275 (2013).

  23. 23.

    et al. Modulation of NADH levels by Arabidopsis Nudix hydrolases, AtNUDX6 and 7, and the respective proteins themselves play distinct roles in the regulation of various cellular responses involved in biotic/abiotic stresses. Plant Cell Physiol. 57, 1295–1308 (2016).

  24. 24.

    et al. Molecular characterization of organelle-type Nudix hydrolases in Arabidopsis. Plant Physiol. 148, 1412–1424 (2008).

  25. 25.

    et al. Identification of novel plant peroxisomal targeting signals by a combination of machine learning methods and in vivo subcellular targeting analyses. Plant Cell 23, 1556–1572 (2011).

  26. 26.

    et al. Activation of NADPH-recycling systems in leaves and roots of Arabidopsis thaliana under arsenic-induced stress conditions is accelerated by knock-out of Nudix hydrolase 19 (AtNUDX19) gene. J. Plant Physiol. 192, 81–89 (2016).

  27. 27.

    et al. The Pfam protein families database: towards a more sustainable future. Nucleic Acids Res. 44, D279–D285 (2016).

  28. 28.

    et al. Studies on the ADP-ribose pyrophosphatase subfamily of the nudix hydrolases and tentative identification of trgB, a gene associated with tellurite resistance. J. Biol. Chem. 274, 32318–32324 (1999).

  29. 29.

    et al. A comprehensive bioinformatics analysis of the Nudix superfamily in Arabidopsis thaliana. Comp. Funct. Genomics 2009, 820381 (2009).

  30. 30.

    et al. CyanoBase: the cyanobacteria genome database update 2010. Nucleic Acids Res. 38, D379–D381 (2010).

  31. 31.

    et al. Molecular evolution of the ocnus and janus genes in the Drosophila melanogaster species subgroup. Mol. Biol. Evol. 18, 801–811 (2001).

  32. 32.

    & Progress in chlorophyll fluorescence research: major developments during the past years in retrospect. Prog. Bot. 54, 151–173 (1993).

  33. 33.

    & Controlling the false discovery rate: a practical and powerful approach to multiple testing. J. R. Stat. Soc. Series B 57, 298–300 (1995).

  34. 34.

    et al. Arabidopsis WRKY38 and WRKY62 transcription factors interact with histone deacetylase 19 in basal defense. Plant Cell 20, 2357–2371 (2008).

  35. 35.

    et al. CBP60g and SARD1 play partially redundant critical roles in salicylic acid signaling. Plant J. 67, 1029–1041 (2011).

  36. 36.

    & Cross talk between signaling pathways in pathogen defense. Curr. Opin. Plant Biol. 5, 325–331 (2002).

  37. 37.

    et al. Antagonistic interaction between systemic acquired resistance and the abscisic acid-mediated abiotic stress response in Arabidopsis. Plant Cell 20, 1678–1692 (2008).

  38. 38.

    et al. The first characterised wheat (Triticum aestivum L.) member of the nudix hydrolase family shows specificity for NAD(P)(H) and FAD. J. Cereal Sci. 51, 319–325 (2010).

  39. 39.

    et al. The redox state of the NADP system in illuminated chloroplasts. Biochim. Biophys. Acta 637, 530–539 (1981).

  40. 40.

    et al. Redox Transfer across the Inner Chloroplast Envelope Membrane. Plant Physiol. 95, 1131–1137 (1991).

  41. 41.

    & Compartmentation and reduction of pyridine nucleotides in relation to photosynthesis. Biochim. Biophys. Acta 109, 390–408 (1965).

  42. 42.

    et al. On the mechanism of effector-mediated activation of ribulose bisphosphate carboxylase/oxygenase. J. Biol. Chem. 256, 6623–6628 (1981).

  43. 43.

    et al. Crystal structure of rice Rubisco and implications for activation induced by positive effectors NADPH and 6-phosphogluconate. J. Mol. Biol. 422, 75–86 (2012).

  44. 44.

    et al. Pleiotropic modulation of carbon and nitrogen metabolism in Arabidopsis plants overexpressing the NAD kinase2 gene. Plant Physiol. 151, 100–113 (2009).

  45. 45.

    et al. Metabolome and photochemical analysis of rice plants overexpressing Arabidopsis NAD kinase gene. Plant Physiol. 152, 1863–1873 (2010).

  46. 46.

    et al. Controlled levels of salicylic acid are required for optimal photosynthesis and redox homeostasis. J. Exp. Bot. 57, 1795–1807 (2006).

  47. 47.

    et al. H2O2-triggered retrograde signaling from chloroplasts to nucleus plays specific role in response to stress. J. Biol. Chem. 287, 11717–11729 (2012).

  48. 48.

    & The use of chlorophyll fluorescence nomenclature in plant stress physiology. Photosynth. Res. 25, 147–150 (1990).

  49. 49.

    et al. Contribution of fructose-1,6-bisphosphatase and sedoheptulose-1,7-bisphosphatase to the photosynthetic rate and carbon flow in the Calvin cycle in transgenic plants. Plant Cell Physiol. 47, 380–390 (2006).

  50. 50.

    et al. Characterizing the cancer genome in lung adenocarcinoma. Nature 450, 893–898 (2007).

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Acknowledgements

We are grateful to Azusa Kanamori and Haruka Mukai for their technical assistance. This work was financially supported by the Ministry of Education, Culture, Sports, Science and Technology (MEXT) KAKENHI [Grant-in-Aid for Scientific Research (B) grant No. 16H05070 (to S.S. and K.Y.)], and by the faculty of Life and Environmental Science in Shimane University (T.M.).

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Affiliations

  1. Department of Advanced Bioscience, Faculty of Agriculture, Kindai University, 3327-204 Nakamachi, Nara 631-8505, Japan

    • Takanori Maruta
    • , Takahisa Ogawa
    • , Masaki Tsujimura
    • , Keisuke Ikemoto
    • , Tomofumi Yoshida
    •  & Shigeru Shigeoka
  2. Department of Life Science and Biotechnology, Faculty of Life and Environmental Science, Shimane University, 1060 Nishikawatsu, Matsue, Shimane 690-8504, Japan

    • Takanori Maruta
    •  & Takahisa Ogawa
  3. Graduate School of Horticulture, Chiba University, 648 Matsudo, Matsudo, Chiba 271-8510, Japan

    • Hiro Takahashi
  4. Department of Food and Nutritional Science, College of Bioscience and Biotechnology, Chubu University, 1200 Matsumoto-cho, Kasugai, Aichi 487-8501, Japan (K.Y.)

    • Kazuya Yoshimura

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Contributions

T.M., T.O. and K.Y. designed the study, performed experiments, and analyzed the data. M.T., K.I. and T.Y. performed experiments supervised by T.M., K.Y. and S.S. H.T. analyzed the microarray data. T.M., T.O., K.Y., and S.S. wrote the article with contribution of all coauthors.

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The authors declare no competing financial interests.

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Correspondence to Shigeru Shigeoka.

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