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Article

Proteomics Analysis Reveals Non-Controlled Activation of Photosynthesis and Protein Synthesis in a Rice npp1 Mutant under High Temperature and Elevated CO2 Conditions

by
Takuya Inomata
1,
Marouane Baslam
2,
Takahiro Masui
1,
Tsutomu Koshu
1,
Takeshi Takamatsu
1,2,
Kentaro Kaneko
1,
Javier Pozueta-Romero
3 and
Toshiaki Mitsui
1,2,*
1
Graduate School of Science and Technology, Niigata University, 2-8050 Ikarashi, Niigata 950-2181, Japan
2
Department of Biochemistry, Niigata University, Niigata 950-218, Japan
3
Instituto de Agrobiotecnología (CSIC, UPNA, Gobierno de Navarra), Mutiloako Etorbidea Zenbaki Gabe, 31192 Mutiloabeti, Nafarroa, Spain
*
Author to whom correspondence should be addressed.
Int. J. Mol. Sci. 2018, 19(9), 2655; https://doi.org/10.3390/ijms19092655
Submission received: 15 August 2018 / Revised: 30 August 2018 / Accepted: 3 September 2018 / Published: 7 September 2018
(This article belongs to the Special Issue Plant Proteomic Research 2.0)
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Abstract

:
Rice nucleotide pyrophosphatase/phosphodiesterase 1 (NPP1) catalyzes the hydrolytic breakdown of the pyrophosphate and phosphodiester bonds of a number of nucleotides including ADP-glucose and ATP. Under high temperature and elevated CO2 conditions (HT + ECO2), the npp1 knockout rice mutant displayed rapid growth and high starch content phenotypes, indicating that NPP1 exerts a negative effect on starch accumulation and growth. To gain further insight into the mechanisms involved in the NPP1 downregulation induced starch overaccumulation, in this study we conducted photosynthesis, leaf proteomic, and chloroplast phosphoproteomic analyses of wild-type (WT) and npp1 plants cultured under HT + ECO2. Photosynthesis in npp1 leaves was significantly higher than in WT. Additionally, npp1 leaves accumulated higher levels of sucrose than WT. The proteomic analyses revealed upregulation of proteins related to carbohydrate metabolism and the protein synthesis system in npp1 plants. Further, our data indicate the induction of 14-3-3 proteins in npp1 plants. Our finding demonstrates a higher level of protein phosphorylation in npp1 chloroplasts, which may play an important role in carbohydrate accumulation. Together, these results offer novel targets and provide additional insights into carbohydrate metabolism regulation under ambient and adverse conditions.

Graphical Abstract

1. Introduction

Changes in climate explain a major portion (32–39%) of yield variability, which correspondingly may translate into large fluctuations in global crop production [1]. Climate change that alters photosynthetic rates may modify physiological responses, plant growth rates (and overall productivity), and resource uses. Therefore, the potential for physiological functioning to evolve in response to climate change will be a key indicator of plant resilience in future environments [2,3]. As they are mostly immobile, plants must adapt to their biotic and abiotic environments limiting or promoting productivity and carbon biosequestration. Photosynthesis can be critical to mitigating the effects of changing climatic conditions. Although the relationship between stomatal conductance, CO2 uptake, and photosynthesis fluctuates in nature, leaf photosynthesis is known to be highly correlated with stomatal conductance in rice [4,5]. Studies employing mutants deficient in a stomatal anion channel protein SLAC1 (Slow Anion Channel-associated 1) revealed that stomatal conductance is a major determinant of photosynthetic rate in higher plants [6,7]. Thus, terrestrial plants regulate CO2 uptake by stomatal switch in response to environmental and biochemical stimuli. The assimilated carbon is further converted to starch in the plastid stroma or to sucrose in the cytosol via sugar nucleotides. In rice leaves, it has been shown that the assimilated carbon is partitioned into sucrose rather than starch [8,9]. Under varying environmental conditions, plant growth and development have to be counterbalanced for defense and stress adaption. Notably, proportional changes in protein composition in response to environmental changes are a major cellular response to requirements of homeostatic adjustment and metabolic remodeling.
Starch is synthesized in plant leaves during the day from photosynthetically fixed carbon. It is then mobilized and thus constitutes an important carbon reserve as well as an energy source for plants and provides the major nutritional value of food crops. Starch biosynthesis occurs in plastids and requires several key enzymes [10,11]. Starch, probably the most important metabolite of plant carbohydrate metabolism, is an insoluble polyglucan produced by starch synthase (SS) using ADP-glucose as the sugar donor nucleotide. Among the many enzymes participating in plant nucleotide catabolism, the pyrophosphatase/phosphodiesterase (NPP) family members, including NPP1, actively catalyze the hydrolytic breakdown of the pyrophosphate and phosphodiester bonds of ADP-glucose [12,13,14]. In rice, six NPP genes (NPP1–6) have been identified and characterized [14]. The NPP genes are located on chromosomes 3 (NPP3), 8 (NPP1), 9 (NPP6), and 12 (NPP2, 4, 5) in the rice genome. Although NPP3 was exclusively localized in the endomembrane system [15], NPP1, 2, and 6 exhibited a dual localization in both the plastid and endomembrane systems [13,16,17], as has been found for other plastidial glycoproteins [18,19,20,21,22]. Whereas NPP1 and NPP6 recognized nucleotide sugars, NPP2 did not recognize these compounds as substrates but preferentially hydrolyzed uridine diphosphate (UDP), ADP, and adenosine 5′-phosphosulfate (APS). NPP1 best hydrolyzed ADP-glucose, ADP-ribose, and ATP, while ADP and ADP-glucose were the best substrates for NPP6. Rice NPP genes showed tissue- and stage-specific expression [14,15]. Thus, it is possible to suppose that rice NPPs are engaged in multiple biological functions through the influence of the turnover of nucleotides and nucleotide derivatives. NPP1 is a major determinant of ADP-glucose pyrophosphatase (AGPPase) activity and can reduce the plastidic pool of ADP-glucose required for starch accumulation in rice [14]. Plant NPPs seem to play a crucial role in carbon flux by transporting carbon taken up from starch and from cell wall polysaccharide biosynthesis to other metabolic pathways in response to the physiological needs of the cell. We have previously shown that when the npp1 null mutant is grown under different CO2 concentration and temperature conditions, NPP1 exerts a negative effect on plant growth and starch accumulation. This provided the first in vivo evidence for the role of NPP1 in the control of growth and reserve pool of carbohydrate in rice under fluctuating climatic conditions [14]. Recently, the presence of NPPs in the plastidial compartment was further confirmed [13,15,16]. Moreover, we have tentatively identified complex-type and pauci-mannosidic-type oligosaccharide chains with β1,2-xylose and/or differential core α1,3-fucose residue(s) in rice NPP1, which provides strong evidence that the trans-Golgi compartments participate in the Golgi-to-plastid trafficking and targeting mechanism of NPP in rice [16]. Plants with a defective endoplasmic reticulum (ER) N-glycosylation pathway and N-glycan maturation are associated with diverse phenotypes and are more sensitive to environmental conditions [23]. Nonetheless, the regulatory mechanisms of high temperature and elevated CO2-induced starch accumulation and growth stimulation in npp1 leaves are unknown. Herein, we highlight that the loss-of-function of NPP1 not only influences stomatal conductance, photosynthesis, and plants’ storage of starch and sucrose but also impacts a set of proteins involved in carbohydrate metabolism and the protein synthetic system in rice leaves under high temperature and CO2 conditions (HT + ECO2).

2. Results and Discussion

2.1. Knocking out NPP1 Decreases Leaf Temperature and Enhances Stomatal Conductance under High Temperature and Elevated CO2 Conditions

In order to examine phenotypic characteristics of the npp1 mutant, 60-day old wild-type (WT) and npp1 mutant rice plants were subjected to thermographic analysis in a spacious Biotron (length 4.5 × width 4.5 × height 1.8–2.2 m) with varying temperatures (28 and 33 °C) and CO2 concentrations (40 and 160 Pa) under natural sunlight. As shown in Figure 1, the leaf temperatures of WT and npp1 plants increased concomitantly with the CO2 concentration irrespective of temperature conditions. Notably, the leaf temperature in npp1 plants was apparently lower than in WT plants at all temperature and CO2 conditions examined (Figure 1). We further examined the flag leaves’ temperatures in WT and npp1 under the different temperature (28 and 33 °C) and CO2 conditions (40 to 200 Pa) under fully controlled environmental chamber conditions (width 64 × width 56 × height 108 cm) using a portable photosynthesis measuring system (Figure 2A). The leaf temperatures of both WT and npp1 gradually increased as CO2 concentrations increased, irrespective of temperature conditions, and reached saturation at 160 Pa (Figure 2A).
The reduction of leaf temperature in npp1 strongly suggested that knocking out NPP1 increases the transpiration rate of the plant. This inference was corroborated by the analysis of the stomatal conductance (gs) under varying temperatures and CO2 concentrations. As shown in Figure 2B, elevated CO2 concentrations caused partial stomatal closure in the two genotypes. No significant differences were observed in the gs values between the two temperature regimes. Notably, the gs values in npp1 plants were higher than in WT plants under all temperatures and CO2 concentrations.
Previous reports have shown that high CO2 decreases gs in a temperature-independent manner [6,24,25,26,27,28]. Changes in gs value in the npp1 mutant under different temperature and CO2 conditions were similar to those in WT, indicating that the stomatal regulatory mechanisms of npp1 work normally.

2.2. Knocking out NPP1 Enhances Photosynthetic Capacity under High Temperature and Elevated CO2 Conditions

The high gs values observed in the npp1 mutant suggested that the lack of NPP1 expression enhances CO2 diffusion. In line with this presumption we found that, irrespective of the temperature regime, the intercellular-to-atmospheric CO2 mole fraction (Ci/Ca) in npp1 was higher than in WT plants at all atmospheric CO2 concentrations (Figure 2C). Consistently, npp1 plants had higher net rates of CO2 assimilation (An) than WT plants at all atmospheric CO2 levels in the two temperature regimes (Figure 2D).
Whether enhanced photosynthesis in npp1 plants is solely the consequence of enhanced CO2 diffusion was investigated by measuring An under varying Ci. As shown in Figure 3, these analyses revealed that the npp1 mutant showed higher An values than WT plants at all Ci levels. In rice plants, sucrose is the primary transport sugar and plays a central role in plant growth and development. As expected, levels of sucrose in npp1 mutants were found to be significantly higher compared with their control WT in any incubation conditions (Figure 4). Previously, the npp1 mutants have been shown to accumulate starch under high CO2 concentration conditions [14]. Thus, it is evident that NPP1 exerts a negative effect on carbohydrate accumulation under HT + ECO2. In these conditions, the npp1 mutants increase photosynthesis and the Calvin-Benson cycle (as detailed below), the latter via increased accumulation of Rubisco activase, enabling npp1 plants to adjust downstream reactions such as sucrose biosynthesis and phloem loading to the increased leaf assimilation. These results indicate that the stimulation of photosynthesis in the npp1 mutant was caused by both stomatal conductance and non-stomatal conductance related causes. Stomata opening and closure occurs via changes in the turgor pressure of guard cells, and the physiological event is regulated by ion and sugar movements in the guard cells [6,29,30]. Increased CO2 concentrations enhance anion channel activity (which has been proposed to be a means of mediating the efflux of osmoregulatory anions from guard cells) [31], causing stomatal closure in rice leaves (Figure 2B, [32]). In npp1 guard cells, the accumulation of sucrose probably causes stomata opening, further activating the photosynthesis of npp1 leaves under the elevated CO2. The NPP1 enzyme, which hydrolyzes sugar nucleotides and ATP, is localized and functions in the chloroplast of rice, therefore, the contents of ATP in chloroplasts should be increased. The high level of ATP in npp1 chloroplasts would boost the turnover of the Calvin cycle and actively convert CO2 to starch and sucrose. In fact, in npp1 null mutants grown under different temperature conditions and CO2 concentrations, a negative effect on the reserve pool of carbohydrates is seen. In this case, NPP activity may occupy a central position in carbon metabolism and its metabolic output to provide products such as the amino acids and lipids necessary for increasing plant biomass.

2.3. Proteomic Characterization of npp1 Leaves under High Temperature and Elevated CO2 Conditions

To characterize changes in the proteome of npp1 leaves under HT + ECO2, we carried out a quantitative proteomic analysis. Proteins extracted from leaves of WT and npp1 plants grown under normal (28/23 °C and 40 Pa CO2) and HT + ECO2 (33/28 °C and 160 Pa CO2) conditions were labeled by iTRAQ (isobaric tag for relative and absolute quantitation), followed by tandem mass spectrometry (MS/MS) analysis. Using this approach, 103 differentially expressed proteins were successfully identified among 1701 detected proteins in total. The general trend indicates that the response of the npp1 mutant to the HT + ECO2 treatment is due, at least partly, to changes in the expression of proteins from the following groups: photosynthesis, carbohydrate metabolism, protein synthesis, and signaling.

2.4. Photosynthesis and Carbohydrate Metabolism

Various proteins associated with photosynthesis and carbohydrate metabolism were upregulated in HT + ECO2 grown npp1 plants (Figure 5A) compared with WT plants (Figure 5B). The HT + ECO2 treatment promoted the expression of Rubisco activase, a protein that acts as Rubisco’s catalytic chaperone [33]. This result is consistent with the enhanced photosynthetic carbon assimilation and also a rise in electron transport capacity. Growth under HT + ECO2 also upregulated the expression of Calvin-Benson enzymes (e.g., fructose-bisphosphate aldolase (FBPA), phosphoglycerate kinase (PGK), and phosphoribulokinase (PRK)). The data presented thus indicate that the HT + ECO2 enhancement of photosynthesis in npp1 is the result of enhanced enzymatic activities involved in CO2 fixation.
The starch synthesis-related enzymes, G1P adenylyltransferase (AGPase), sucrose synthase (SuSy), and 4-α-glucanotransferase protein (DPE2), exhibited a clear upregulation under HT + ECO2. AGPase is produced from ATP and glucose 1-phosphate to the ADP-glucose necessary for starch biosynthesis. SuSy is responsible for the conversion of sucrose and a nucleoside diphosphate into the corresponding nucleoside diphosphate glucose and fructose, however, this sucrolytic protein may participate in the direct conversion of sucrose into ADP-glucose linked to starch biosynthesis. The sucrose and starch metabolic pathways are tightly interconnected by means of cytosolic ADP-glucose producing enzymes such as SuSy and by the action of an ADP-glucose translocator located on the chloroplast envelope membranes [10,34]. Furthermore, the levels of cytosolic glucanotransferase DPE2 involved in the conversion of starch into sucrose [35] were high in npp1 leaves under HT + ECO2 conditions. The high expression of AGPase, SuSy, and DPE2 induced under HT + ECO2 conditions would be crucial factors for carbohydrate accumulation.

2.5. Protein Synthesis System

The marked upregulation of a large set of proteins related to the protein synthesis system when knocking out npp1 was also produced by the enhancement of temperature and CO2 (Figure 5C), although such an increase was not observed in WT leaves (Figure 5D). Ribosome components such as 60S, 50S, 40S, and 30S ribosomal proteins were identified as being upregulated. In addition, elongation factor 1 (EF-Iα and β), 2, T (EF-Ts and -Tu), and four rice eukaryotic initiation factor proteins (eIF 3A, eIF 3F, eIF4A, and eIF4F) were increased in npp1 under HT + ECO2. EF-Iα controls GTP-binding proteins responsible for cytoskeletal tubulin, which is positively correlated with starch accumulation [36]. Early studies showed that EF-Iα can influence the organization of cytoskeletal components surrounding protein bodies around the endoplasmic reticulum membranes, which appear to reorganize coincident with the actively accumulating storage proteins in the endosperm [37]. eIF participates in most translation initiation processes and plays important roles in the growth and development (and organ size) of Arabidopsis and rice [38,39,40].

2.6. Signaling

Several 14-3-3 proteins exhibited significant changes in npp1 mutants under HT + ECO2 conditions (Figure 6) and were thus deemed to play important roles in starch biosynthesis in rice leaves. In this study, the upregulation of three 14-3-3 isoforms (14-3-3 GF14C, 14-3-3 GF14E, and 14-3-3 GF14F) was detected, suggesting changes in the phosphorylation status in npp1 mutants. Recently, the ectopic overexpression of the cassava 14-3-3 gene in Arabidopsis showed an increase in starch content in the leaves from transgenic plants [36]. A striking feature of the 14-3-3 proteins is their ability to bind a multitude of functionally diverse signaling proteins, including kinases, phosphatases, and transmembrane receptors [41], and 14-3-3 proteins play roles in regulating plant development and stress responses by effecting direct protein-protein interactions [42,43,44]. The interactions with 14-3-3s are subject to environmental control through signaling pathways that impact on 14-3-3 binding sites. The phosphoserine/threonine-binding 14-3-3 proteins participate in environmentally responsive phosphorylation-linked regulatory functions in plants and are potentially involved in starch regulation [45]. Previous studies have identified the protein-protein interactions between 14-3-3 and key enzymes of primary metabolism (e.g., sucrose-phosphate synthase and glyceraldehyde-3-phosphate dehydrogenase) and showed the central role of 14-3-3s as regulators of enzymes of cytosolic metabolism and ion pumps [46,47,48,49]. A molecular genetic analysis of 14-3-3 isoforms using overexpressed and knockout plants with studies of protein-protein interactions revealed alterations in the level of metabolic intermediates of glycolysis, tricarboxylic acid (TCA), and biosynthesis of aromatic compounds [50]. Hence, we may speculate that 14-3-3 may play a role in the accumulation of starch in npp1 mutants by interacting with metabolic enzymes and thus appears to maintain those enzymes in an active state in the cell. Notably, 14-3-3 proteins have been localized to the chloroplast stroma and the stromal side of thylakoid membranes [51], thereby implicating a potential role in starch regulation.
Photosynthesis, sugar assays, and quantitative proteomic analyses of leaves of knockout npp1 revealed that the mutant plants always become highly active regardless of normal or HT and ECO2 conditions (Figure 3, Figure 4 and Figure 5). The higher An in npp1 mutants could be the consequence of various factors: (i) higher CO2 diffusion; (ii) more efficient conversion of light energy into ATP; and (iii) the upregulation of photosynthetic enzymes (Rubisco activase and Calvin-Benson enzymes). We consider that an activation effector would be the high level of ATP in chloroplasts, since NPP1 preferentially hydrolyzes ATP [14]. Of note, a series of 14-3-3 proteins were upregulated in npp1 mutants (Figure 6), suggesting that the protein phosphorylation status is possibly changed by the disruption of the NPP1 gene. Phosphorylation of proteins in chloroplasts plays a major role in regulating both the light and dark reactions of photosynthesis. Light-harvesting chlorophyll a/b binding proteins [52,53,54], Rubisco [55], Rubisco activase [56], phosphoglycerate kinase [57], Glyceraldehyde 3-phosphate dehydrogenase (GAPDH) [58], and transketolase [59] were shown to be phosphorylated and the enzyme functions were regulated. In addition, sigma factor [60] and 24/28 RNA binding proteins [61] were also phosphorylated.
We analyzed the phosphorylation state of WT and npp1 chloroplast proteins under HT and ECO2 conditions by employing TiO2 chromatography and mass spectrometry. The phosphopeptides derived from chlorophyll a/b binding protein, Rubisco large chain, pyruvate phosphate dikinase, and some other plastidial enzymes and proteins were detected with good reproducibility. The level of protein phosphorylation in npp1 chloroplasts under HT and ECO2 was higher than that of npp1 under the normal condition or the WT chloroplasts (Table 1). The chlorophyll a/b binding protein is the main component of the light-harvesting complex (LHC), which is a light receptor that captures and delivers excitation energy to photosystems PSI and PSII. The reversible phosphorylation of light harvesting chlorophyll a/b binding proteins (LHCII) has been observed, which regulates state transitions for balancing the excitation energy between PSI and PSII [54,62]. As shown in Table 1, several phosphorylation sites of chlorophyll a/b binding proteins in the npp1 mutant were more highly phosphorylated in comparison with the WT chloroplasts. In addition, the phosphorylation level of chlorophyll a/b binding proteins in both npp1 and WT were increased under HT and ECO2 conditions. In our phosphoproteomic analysis, two phosphopeptides plastid movement impaired1 (PMI1) and plastid transcriptionally active 16 (pTac16) were found to be more abundant under ECO2 + HT condition in npp1 mutant plants. The PMI1 is a plant-specific C2-domain protein that plays a role in organelle movement and positioning [63]. The movements of npp1 organelles (i.e chloroplasts) within the cell, which become appropriately positioned under ECO2 + HT, could be a fundamental cellular activity to accomplish their functions and adapt to environmental stress. The pTac16 is a plastid membrane-attached multimeric protein complex involved in plastid transcription and translation. The knockout lines ptac seedlings developed white or yellow cotyledons, failed to accumulate chlorophyll even under low light intensities, impaired plastid structure [64], and downregulated levels of plastid-encoded polymerase (PEP) responsible exclusively for the expression of chloroplast-encoded photosynthetic genes [65,66]. The upregulation of pTac 16 in npp1 mutant plants under HT + ECO2 could at least partly explain the enhancement of photosynthesis-related genes and activity, and plastid metabolism. Hence, we consider that the high phosphorylation status in npp1 under HT and ECO2 could be related to the activation of growth and carbohydrate accumulation of the seedlings.

3. Material and Methods

3.1. Plant Material and Growth Condition

The rice variety used in this study was Oryza sativa L. cv. Nipponbare. The Tos17-inserted line of NPP1 (ND8012) was obtained from the National Institute of Agrobiological Sciences (NIAS, Tsukuba, Japan; [67]), and the npp1-1-1 line with a single copy of Tos17 inserted into the NPP1 gene was established previously. WT and npp1 mutant plants were grown and harvested at Niigata University paddy field (Niigata, Japan).
WT and npp1 mutant seeds were grown in a commercial soil (Kumiai Gousei Baido 3, JA, Tokyo, Japan) in plastic pots and incubated in the growth chamber (CFH-415, Tomy Seiko, Tokyo, Japan) at 28 °C (14 h day)/23 °C (10 h night) cycles with fluorescent lighting (300 μmol·m–2·s–1). Seeds and plant samples were stored at 4 °C before analysis.

3.2. Thermal Imaging

Thermal images of WT and npp1 mutant plants were obtained using the InfRec (NEC) thermal video system. Plants grown for 60 days on soil (Kumiai Gousei Baido 3) were transferred to Biotron LPH-1.5PH-NCII (length 4.5 × width 4.5 × height 1.8–2.2 m, Nihon-ika, Osaka, Japan) and incubated under four different conditions (28 °C, 40 Pa CO2; 28 °C,160 Pa CO2; 33 °C, 40 Pa CO2; 33 °C/160 Pa CO2) at 70% relative humidity under natural light.

3.3. Gas Exchange Measurements

Photosynthetic rate (An), leaf conductance (gs), and intercellular CO2 concentrations [CO2] (Ci) were measured with a portable photosynthesis LI-6400XL system (LI-6400-20, LiCor Biosciences, Lincoln, NE, USA). Gas exchange of WT and npp1 leaves was recorded in the central segment of top leaves attached to the main culm between 3 and 8 h after the start of the photoperiod. Leaf cuvette conditions were set as follows: block temperature was set at ambient (growth chamber; 28 °C) and high (33 °C) temperatures; [CO2] was set at 400 to 2000 µmol·mol−1; relative humidity was maintained equal to that in the growth chamber; and Photosynthetically Active Radiation (PAR) was set at 1200 µmol·m−2·s−1, resulting in light-saturated photosynthesis and no decline as a result of photorespiration.

3.4. Assay

Sucrose content was measured according to the methods described previously [18,68]. Chlorophyll extracted from the isolated chloroplasts with 80% (v/v) acetone was assayed by the method described by Porra et al. [69]. Protein concentration was determined by the Pierce 660 nm Protein Assay Kit (Thermo Fisher Scientific, Waltham, MA, USA) using bovine serum albumin (BSA) as a standard.

3.5. Analysis of Leaf Proteome

Two hundred milligrams of leaves of WT and npp1 grown for 7 days under normal (28 °C, 14 h day/23 °C, 10 h night, 40 Pa CO2) and elevated temperature and CO2 (33 °C, 14 h day/28 °C, 10 h night, 160 Pa CO2) conditions were ground in liquid nitrogen and suspended in 7 M urea, 2 M thiourea, 3% (w/v) CHAPS (3-((3-cholamidopropyl) dimethylammonio)-1-propanesulfonate), 1% (v/v) Triton X-100, and 10 mM dithiothreitol. After centrifugation at 10,000× g at 4 °C for 5 min, the supernatants were mixed with 1/10 volume of 100% (w/v) TCA, incubated on ice for 15 min, and then centrifuged at 10,000× g at 4 °C for 15 min. The resulting precipitates were washed three times with ice-cold acetone and resuspended in 8 M urea.
The procedure of quantitative shotgun proteomic analysis was the same as previously described [68]. The protein samples (50 µg) were thoroughly digested with endoproteinase Lys-C and trypsin at 37 °C for 12 h. iTRAQ labeling of peptides was carried out with 4-plex iTRAQ tags according to the manufacturer’s protocol (AB Sciex, Framingham, MA, USA), and the resultant 4-iTRAQ-labeled peptide samples were mixed. iTRAQ analysis was performed by employing a DiNa-A-LTQ-Orbitrap-XL system operated with Xcalibur 2.0 software (Thermo Fisher Scientific). Proteins were identified with Proteome Discoverer v. 1.4 software, and the SEQUEST HT (Thermo Fisher Scientific) and MsAmanda [70] search tool using the UniProt (http://www.uniprot.org/) O. sativa subsp. japonica database (63,535 proteins) with the following parameters: enzyme, trypsin; maximum missed cleavages site, 2; peptide charge, 2+ or 3+; MS tolerance, 5 ppm; MS/MS tolerance, ±0.5 Da; dynamic modification, carboxymethylation (C), oxidation (H, M, W), iTRAQ 4-plex (K, Y, N-terminus). False discovery rates were <1%.
The mass spectrometry proteomics data (JPST000338) have been deposited in the jPOST repository (https://repository.jpostdb.org/).

3.6. Analysis of Chloroplast Phosphoproteome

The procedure of chloroplast isolation was essentially identical to the method described earlier [16,71]. Rice seeds were germinated and grown for 7 days under normal (28 °C, 14 h day/23 °C, 10 h night, 40 Pa CO2) and elevated temperature and CO2 (33 °C, 14 h day/28 °C, 10 h night, 160 Pa CO2) conditions. Thirty grams of leaves were homogenized with an equal volume of solution A mixture consisting of 50 mM HEPES-KOH pH 7.5, 0.33 M sorbitol, 5 mM MgCl2, 5 mM MnCl2 and 5 mM EDTA (ethylenediaminetetraacetic acid), 50 mM sodium ascorbate, and then the homogenates were passed through four layers of gauze and four layers of Miracloth (Merck, Darmstadt, Germany). The filtrate was layered onto an 80% (v/v) Percoll (Sigma, St.Louis, USA) cushion containing solution A, and centrifuged at 2000× g at 4 °C for 4 min. The crude chloroplasts on the Percoll surface were diluted with more than twice the volume of solution A, then layered onto a discontinuous density gradient consisting of 40% and 80% Percoll solutions. The gradient was centrifuged at 4000× g at 4 °C for 10 min. Intact chloroplasts enriched around the 40%/80% Percoll interface were collected and subjected again to the Percoll gradient centrifugation. Intact chloroplasts were diluted with five times the volume of solution A, and centrifuged at 2000× g at 4 °C for 4 min, followed by chlorophyll and protein extractions.
Analyses of phosphoproteins were carried out according to the method described by Fukuda et al. [72]. Intact chloroplasts were suspended in 7 M urea, 2 M thiourea, 3% (w/v) CHAPS, 1% (v/v) Triton X-100, and 10 mM dithiothreitol. After centrifugation at 10,000× g at 4 °C for 5 min, the supernatants were mixed with 1/10 volume of 100% (w/v) TCA, incubated on ice for 15 min, and then centrifuged at 10,000× g at 4 °C for 15 min. The resulting precipitates were washed three times with ice-cold acetone and resuspended in 8 M urea. The protein preparations (100 µg) were digested with 2% (w/w) endoproteinase Lys-C and trypsin in 25 mM NH4HCO3 and 0.8 M urea at 37 °C for 12 h. The reaction mixtures were dried on a Centrifugal Concentrator (CC-105, Tomy, Japan) and then dissolved in buffer A consisting of 60% (v/v) acetonitrile (ACN), 5% (v/v) glycerol, 0.1% (v/v) Trifluoroacetic acid (TFA). A MonoSpin TiO column (1000 μL: GL Science, Tokyo, Japan) was pre-equilibrated with buffer B consisting of 80% (v/v) ACN, 0.1% (v/v) TFA, followed by buffer A, and the samples were centrifuged at 3000× g for 1 min each. The obtained peptide samples were applied to the tip column and centrifuged at 3000× g for 5 min. The flow-through fraction was applied to the tip column again. Subsequently, the tip column was washed three times with buffer A and centrifuged at 3000× g for 1 min. The binding phosphopeptides were eluted with 100 μL of 5% NH4OH with centrifugation at 1000× g for 5 min. After elution with 5% NH4OH, the tightly binding phosphopeptides were eluted with 100 µL of 1 M (w/v) bis-Tris propane with centrifugation at 1000× g for 1 min. The phosphopeptides eluted with 5% NH4OH solution were dried on a Centrifugal Concentrator and then dissolved in 5% (v/v) formic acid (FA). The phosphopeptides eluted with 1 M bis-Tris propane were acidified with 900 μL of 5% FA and then desalted using a MonoSpin C18 column (GL Sciences, Tokyo, Japan).
Each phospho-peptide fraction was loaded on a HiQ sil C-18 W-3 trap column with buffer C consisting of 0.1% (v/v) FA and 2% (v/v) ACN using a DiNa-A system (KYA Tech., Tokyo, Japan). A linear gradient from 0% to 33% buffer D consisting of 0.1% FA and 80% ACN for 600 min, 33% to 100% D for 10 min and back to 0% D in 15 min was applied, and peptides eluted from the HiQ sil C-18 W-3 column were directly loaded on a MonoCap C18 High Resolution 2000 separation column. The separated peptides were introduced into a LTQ-Orbitrap XL mass spectrometer (Thermo Fisher Scientific, Waltham, MA, USA) with a flow rate of 300 nL·min−1 and an ionization voltage of 1.7–2.5 kV. The mass range selected for MS scan was set to 350–1600 m/z and the top five peaks were subjected to MS/MS analysis. The full MS scan was detected in the Orbitrap, and the MS/MS scans were detected in the linear ion trap. The normalized collision energy for MS/MS was set to 35 eV for collision-induced dissociation (CID).
Operation of protein identification with software and database was carried out as described above [68]. The phosphorylation of S/T/Y and oxidation of H/M/W residues were set as dynamic modifications. False discovery rates were <1%.
The chloroplast phosphoproteome data (JPST000462) have been deposited in the jPOST repository (https://repository.jpostdb.org/).

4. Conclusions

Previous investigations have revealed that NPP1 exerts a negative effect on starch accumulation and growth. NPP1 localizes to the chloroplasts and degrades a number of nucleotides including ADP-glucose and ATP, thus, it is possibly a kind of room (for example, chloroplast stroma) cleaning enzyme. The molecular physiological phenotype of the npp1 mutant was further analyzed in the present study. Lower temperatures and changes in the transpiration rates of npp1 leaves were observed, indicating that the disruption of the NPP1 gene caused the stomatal opening of rice leaves. Furthermore, the analysis of the An/Ci curve indicated that the enhancement of photosynthesis in npp1 resulted from multiple causes in addition to the stomatal conductance. The proteome of carbohydrate metabolism and protein synthesizing system in npp1 leaves was strongly upregulated by HT and ECO2. Furthermore, the protein phosphorylation status in npp1 chloroplasts was significantly higher than in WT chloroplasts. An increase in ATP in chloroplasts might be a key stimulus, because NPP1 preferentially hydrolyzes ATP. Judging from the overall results, we consider that the remarkable enhancement of plant growth and carbohydrate accumulation in npp1 mutant plants under HT and ECO2 conditions was a consequence of the non-controlled activation of photosynthesis and protein synthesis by loss of function of a fine-tuning enzyme NPP1.

Author Contributions

T.M. (Toshiaki Mitsui) conceived and designed the project. T.I., T.M. (Takahiro Masui), K.K., T.K., and T.T. (Toshiaki Mitsui) performed the experiments. T.M. (Toshiaki Mitsui) and M.B. supervised and interpreted the data. T.M., M.B., and J.P.-R. wrote the manuscript. All authors discussed the results and implications and commented on the manuscript at all stages.

Funding

This research was supported by Grants-in-Aid for Scientific Research (A) (15H02486) and Strategic International Collaborative Research Program by the Japan Science and Technology Agency (JST SICORP).

Conflicts of Interest

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

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Figure 1. Leaf temperatures of WT and npp1 mutant plants under different temperatures and CO2 concentrations in Biotron’s environmental conditions. WT (filled bars) and npp1 (open bars) plants grown for 60 days under normal conditions (14 h light/10 h dark: 28/23 °C, 40 Pa CO2) after germination were subjected to thermographic analysis of their leaf temperatures under different temperature and CO2 conditions: (A) 28 °C, 40 Pa, (B) 28 °C, 160 Pa, (C) 33 °C, 40 Pa, and (D) 33 °C, 160 Pa. Values in upper panel show the means ± standard deviation (s.d.) (n = 5). Asterisks indicate significant differences by Student’s t-test (*, p > 0.05; **, p > 0.01). Lower panels represent the thermographic images. WT: wild-type.
Figure 1. Leaf temperatures of WT and npp1 mutant plants under different temperatures and CO2 concentrations in Biotron’s environmental conditions. WT (filled bars) and npp1 (open bars) plants grown for 60 days under normal conditions (14 h light/10 h dark: 28/23 °C, 40 Pa CO2) after germination were subjected to thermographic analysis of their leaf temperatures under different temperature and CO2 conditions: (A) 28 °C, 40 Pa, (B) 28 °C, 160 Pa, (C) 33 °C, 40 Pa, and (D) 33 °C, 160 Pa. Values in upper panel show the means ± standard deviation (s.d.) (n = 5). Asterisks indicate significant differences by Student’s t-test (*, p > 0.05; **, p > 0.01). Lower panels represent the thermographic images. WT: wild-type.
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Figure 2. Changes in temperatures, gs, Ci/Ca, and An of WT and npp1 mutant plants under different temperatures and CO2 concentrations in a controlled growth chamber. Top leaves of main culm of WT (■) and npp1 (□) plants grown for 60 days under normal conditions (14 h light/10 h dark: 28/23 °C, 40 Pa CO2) were subjected to measurements of temperature (A), stomatal conductance to water (gs) (B), ratios of internal [CO2] to ambient [CO2] (Ci/Ca) (C), and photosynthetic rates (An) (D) under the following conditions: temperature, 28 and 33 °C; CO2, 40 to 200 Pa; relative humidity, 50%; light, 1000 μmol·photons·m−2·s−1. Values show the means ± s.d. (n = 3).
Figure 2. Changes in temperatures, gs, Ci/Ca, and An of WT and npp1 mutant plants under different temperatures and CO2 concentrations in a controlled growth chamber. Top leaves of main culm of WT (■) and npp1 (□) plants grown for 60 days under normal conditions (14 h light/10 h dark: 28/23 °C, 40 Pa CO2) were subjected to measurements of temperature (A), stomatal conductance to water (gs) (B), ratios of internal [CO2] to ambient [CO2] (Ci/Ca) (C), and photosynthetic rates (An) (D) under the following conditions: temperature, 28 and 33 °C; CO2, 40 to 200 Pa; relative humidity, 50%; light, 1000 μmol·photons·m−2·s−1. Values show the means ± s.d. (n = 3).
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Figure 3. Photosynthetic rates at different intracellular [CO2] (An /Ci curve) of leaves from WT (■) and npp1 (□) plants. The results of Figure 2 were used to draw an An/Ci curve. Open and filled arrows represent the data obtained at Ca of 40 and 160 Pa, respectively.
Figure 3. Photosynthetic rates at different intracellular [CO2] (An /Ci curve) of leaves from WT (■) and npp1 (□) plants. The results of Figure 2 were used to draw an An/Ci curve. Open and filled arrows represent the data obtained at Ca of 40 and 160 Pa, respectively.
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Figure 4. Sucrose accumulation in leaves of WT and npp1 mutant plants. WT (filled bars) and npp1 (open bars) plants grown for 60 days under normal conditions (28/23 °C, 40 Pa CO2) were further incubated under different temperatures and CO2 concentrations. At the end of a light cycle, the leaves of the WT and the npp1 mutant plants were subjected to sucrose assays. Values show the means ± s.d. (n = 3~5). Asterisks indicate significant differences by Student’s t-test (*, p > 0.05; **, p > 0.01).
Figure 4. Sucrose accumulation in leaves of WT and npp1 mutant plants. WT (filled bars) and npp1 (open bars) plants grown for 60 days under normal conditions (28/23 °C, 40 Pa CO2) were further incubated under different temperatures and CO2 concentrations. At the end of a light cycle, the leaves of the WT and the npp1 mutant plants were subjected to sucrose assays. Values show the means ± s.d. (n = 3~5). Asterisks indicate significant differences by Student’s t-test (*, p > 0.05; **, p > 0.01).
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Figure 5. Changes in the expression of carbohydrate- and protein synthesis-related proteins in leaves of WT and npp1 mutant plants under high temperature and elevated CO2 concentrations. The leaves of WT (B,D) and npp1 (A,C) plants were incubated under normal (28/23 °C, 40 Pa CO2) and HT + ECO2 (33/28 °C, 160 Pa CO2) conditions, and then subjected to a proteomic analysis with Isobaric tags for relative and absolute quantitation (iTRAQ) labeling. Values show the means ± s.d. (n = 3). The red line shows the ratio between HT+ECO2/normal condition mean equal to 1.
Figure 5. Changes in the expression of carbohydrate- and protein synthesis-related proteins in leaves of WT and npp1 mutant plants under high temperature and elevated CO2 concentrations. The leaves of WT (B,D) and npp1 (A,C) plants were incubated under normal (28/23 °C, 40 Pa CO2) and HT + ECO2 (33/28 °C, 160 Pa CO2) conditions, and then subjected to a proteomic analysis with Isobaric tags for relative and absolute quantitation (iTRAQ) labeling. Values show the means ± s.d. (n = 3). The red line shows the ratio between HT+ECO2/normal condition mean equal to 1.
Ijms 19 02655 g005aIjms 19 02655 g005b
Ijms 19 02655 g006 550
Figure 6. Changes in expression of 14-3-3 proteins in leaves of WT and npp1 mutant plants under high temperature and elevated CO2 concentrations. Details of incubation conditions via a proteomic analysis were described in Figure 5. The leaves of WT (filled bars) and npp1 (open bars) plants were incubated under normal and HT + ECO2 conditions. Values show the means ± s.d. (n = 3). Asterisks indicate significant differences by Student’s t-test (**, p > 0.01).
Figure 6. Changes in expression of 14-3-3 proteins in leaves of WT and npp1 mutant plants under high temperature and elevated CO2 concentrations. Details of incubation conditions via a proteomic analysis were described in Figure 5. The leaves of WT (filled bars) and npp1 (open bars) plants were incubated under normal and HT + ECO2 conditions. Values show the means ± s.d. (n = 3). Asterisks indicate significant differences by Student’s t-test (**, p > 0.01).
Ijms 19 02655 g006
Table
Table 1. Phosphopeptide detection in WT and npp1 chloroplasts with or without HT and ECO2 treatment. n.d.: not detected.
Table 1. Phosphopeptide detection in WT and npp1 chloroplasts with or without HT and ECO2 treatment. n.d.: not detected.
DescriptionAccessionWT ControlWT HT&ECO2npp1 Controlnpp1 HT&ECO2
Chlorophyll a/b-binding proteinQ6Z411(1.15 ± 0.78) × 108(2.43 ± 2.06) × 108(1.05 ± 0.53) × 109(7.43 ± 4.27) × 108
Chlorophyll a-b binding protein 2P12331n.d.(4.84 ± 2.39) × 106n.d.(4.29 ± 4.18) × 106
Chlorophyll a-b binding proteinQ7XV11(1.71 ± 1.01) × 106(3.83 ± 0.95) × 106(1.10 ± 0.44) × 107(9.44 ± 4.78) × 106
Ribulose bisphosphate carboxylase large chainP0C512(1.08 ± 0.97) × 107n.d.(1.52 ± 0.29) × 107(1.04 ± 0.78) × 107
ATP synthase subunit betaP12085(3.65 ± 2.51) × 106n.d.n.d.n.d.
PLASTID TRANSCRIPTIONALLY ACTIVE 16Q0DJF9(2.55 ± 1.90) × 107(2.05 ± 1.54) × 107(0.81 ± 1.17) × 107(5.19 ± 7.87) × 107
protein CURVATURE THYLAKOID 1AQ5Z6P4(8.76 ± 1.51) × 107(3.11 ± 0.67) × 107(2.55 ± 0.04) × 107(6.79 ± 4.23) × 107
PLASTID MOVEMENT IMPAIRED1Q0IZR7n.d.n.d.n.d.(4.16 ± 1.49) × 106
Pyruvate, phosphate dikinase 1Q6AVA8(3.35 ± 2.78) × 105(4.62 ±0.02) × 105(1.35 ± 1.24) × 106n.d.

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Inomata, T.; Baslam, M.; Masui, T.; Koshu, T.; Takamatsu, T.; Kaneko, K.; Pozueta-Romero, J.; Mitsui, T. Proteomics Analysis Reveals Non-Controlled Activation of Photosynthesis and Protein Synthesis in a Rice npp1 Mutant under High Temperature and Elevated CO2 Conditions. Int. J. Mol. Sci. 2018, 19, 2655. https://doi.org/10.3390/ijms19092655

AMA Style

Inomata T, Baslam M, Masui T, Koshu T, Takamatsu T, Kaneko K, Pozueta-Romero J, Mitsui T. Proteomics Analysis Reveals Non-Controlled Activation of Photosynthesis and Protein Synthesis in a Rice npp1 Mutant under High Temperature and Elevated CO2 Conditions. International Journal of Molecular Sciences. 2018; 19(9):2655. https://doi.org/10.3390/ijms19092655

Chicago/Turabian Style

Inomata, Takuya, Marouane Baslam, Takahiro Masui, Tsutomu Koshu, Takeshi Takamatsu, Kentaro Kaneko, Javier Pozueta-Romero, and Toshiaki Mitsui. 2018. "Proteomics Analysis Reveals Non-Controlled Activation of Photosynthesis and Protein Synthesis in a Rice npp1 Mutant under High Temperature and Elevated CO2 Conditions" International Journal of Molecular Sciences 19, no. 9: 2655. https://doi.org/10.3390/ijms19092655

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