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BMC Plant Biology

Open Access

Proteomic analysis of proteins related to rice grain chalkiness using iTRAQ and a novel comparison system based on a notched-belly mutant with white-belly

  • Zhaomiao Lin1,
  • Xincheng Zhang1,
  • Xiaoyu Yang1,
  • Ganghua Li1,
  • She Tang1,
  • Shaohua Wang1,
  • Yanfeng Ding1, 2 and
  • Zhenghui Liu1, 2Email author
BMC Plant Biology201414:163

https://doi.org/10.1186/1471-2229-14-163

Received: 9 December 2013

Accepted: 6 June 2014

Published: 12 June 2014

Abstract

Background

Grain chalkiness is a complex trait adversely affecting appearance and milling quality, and therefore has been one of principal targets for rice improvement. Eliminating chalkiness from rice has been a daunting task due to the complex interaction between genotype and environment and the lack of molecular markers. In addition, the molecular mechanisms underlying grain chalkiness formation are still imperfectly understood.

Results

We identified a notched-belly mutant (DY1102) with high percentage of white-belly, which only occurs in the bottom part proximal to the embryo. Using this mutant, a novel comparison system that can minimize the effect of genetic background and growing environment was developed. An iTRAQ-based comparative display of the proteins between the bottom chalky part and the upper translucent part of grains of DY1102 was performed. A total of 113 proteins responsible for chalkiness formation was identified. Among them, 70 proteins are up-regulated and 43 down-regulated. Approximately half of these differentially expressed proteins involved in central metabolic or regulatory pathways including carbohydrate metabolism (especially cell wall synthesis) and protein synthesis, folding and degradation, providing proteomic confirmation of the notion that chalkiness formation involves diverse but delicately regulated pathways. Protein metabolism was the most abundant category, accounting for 27.4% of the total differentially expressed proteins. In addition, down regulation of PDIL 2–3 and BiP was detected in the chalky tissue, indicating the important role of protein metabolism in grain chalkiness formation.

Conclusions

Using this novel comparison system, our comprehensive survey of endosperm proteomics in the notched-belly mutant provides a valuable proteomic resource for the characterization of pathways contributing to chalkiness formation at molecular and biochemical levels.

Keywords

RiceGrain chalkinessiTRAQWhite-bellyNotched-belly mutants

Background

Chalkiness is the opaque part of rice grain. Chalky grains have a lower density of starch granules compared to vitreous ones, and are more prone to breakage during milling. It is also detracts from the visual appearance, adversely affecting consumer acceptability and lowering the overall market value [1]. In many rice-producing areas, high ratio of chalky grains is a major concern that decreases grain quality. For China as an example, many early-season indica and japonica varieties are of high grain chalkiness [2]. Therefore, eliminating chalkiness from rice grain has been one of the prime goals in rice breeding.

High temperatures as well as the combination of high relative humidity and low vapor pressure deficit during grain filling has been shown as the most important environmental conditions affecting grain chalkiness [3]. Current grain filling temperatures are already approaching critical levels in many rice growing counties, resulting in high occurrence of grain chalkiness, currently a major problem for rice production in Asian countries [4]. Therefore, understanding of the mechanisms of grain chalking is indispensable to develop a strategy for reducing the high rate of chalky grains under the likely scenario of global warming.

Grain chalkiness is a complex trait controlled by quantitative trait loci (QTLs). More than 40 QTLs contributing to the percentages of chalky grains and degrees of endosperm chalkiness have been mapped in the rice genome using F2 segregation populations, chromosome segment substitution lines, or introgression lines [2]. These QTLs distributed across all the 12 rice chromosomes, among which qPGWC-7 and qPGWC-8 have been fine-mapped [2]. However, only few QTLs have been isolated and functionally analyzed, and few genes have been identified [5]. So far, the molecular mechanisms underlying the formation of rice grain endosperm chalkiness still remain poorly understood.

In rice grains, starch is the predominant storage substance, constituting nearly 90% of the total dry mass. Microscopic observation showed that starch granules of the chalky endosperm were loosely packed as compared with those of the translucent part [6]. Thus, the incomplete accumulation of starch has been considered as the main cause for chalkiness formation. Most of studies concerning grain chalkiness have been focused on the genes encoding enzymes involved in starch synthesis or carbon metabolism, such as granule-bound sucrose synthase, pyruvate orthophosphate dikinase, starch-branching enzyme IIb, and debranching enzymes as reviewed by Liu et al.[5].

On the other hand, the role of the other major component of rice endosperm, the proteins, has been underestimated to some extent. Recent data report that other diverse factors especially the proteins are also associated with the opaque phenotype. For example, overexpression of a rice binding protein (BiP) produced an opaque phenotype seed with a floury endosperm [7]. In addition, Lin et al.[8] investigated the effects of high temperature during grain filling on the expression of storage proteins, and found that the chalky grains contained reduced amount of prolamins, implying the relationship between prolamins and chalky structure in rice grains. Collectively, these studies indicate the potential role of protein synthesis or nitrogen metabolism in the formation of grain chalkiness, which needs further investigation.

Proteomics is an effective strategy for directly and globally investigating the protein expression patterns and its respective posttranslational modifications. It has been employed in the studies of grain chalkiness under high temperature [8]. Lin et al.[9] analyzed heat stress response of several different cultivars including high-chalky types, and found that sHSP was positively correlated with the appearance of chalky kernels. Li et al.[10] reported that accumulation of isoforms of PPDK and pullulanase was prone to high night temperature. However, comparative display of protein expression patterns in these studies were performed either between varieties [9] or between grains under different treatments for a given variety [8, 10], which can not avoid the effect of genotype and environment.In this study, a notched-belly mutant with white-belly (DY1102) was used as material, which has high percentage of notched-belly grain. Interestingly, the white-belly only occurs in the bottom part proximal to the embryo, with the upper half part being translucent (Figure 1). Based on this mutant, we developed a novel comparison system that can minimize the influence of genetic backgrounds and growing environment. A comparative proteomic analysis by iTRAQ (isobaric tags for relative and absolute quantification) resulted in detection and identification of a total of 113 proteins responsible for grain chalkiness. Our comprehensive and deep survey of endosperm proteomics in the notched-belly mutants with white-belly should provide an excellent starting material for further elucidating the molecular and biochemical basis of rice grain chalkiness.
Figure 1

Mutant of notched-belly with white-belly near embryo (DY1102). A, The panicle of DY1102; B, Brown rice of DY1102; C, Notched-belly grain without white-belly; D, Notched-belly grain with white-belly in bottom half part proximal to the embryo.

Methods

Plant materials

Wuyujing3 is a benchmark japonica rice variety of China for its high eating quality, while it has weak points such as relatively lower yield potential, susceptibility to rice stripe virus, and high chalky grain rate (usually being above 30%) [6]. In 2007, 2000 g seeds of Wuyujing3 were treated with 0.5% ethyl methane sulfonate (EMS) for 16 hours at room temperature (about 25°C). Before sowing, seeds were soaked for 24 hours and then drained 24 hours. M1 seeds was grown in field and mixed harvested. Selection on grain chalkiness was performed at M3 seeds after harvest of M2 plants in 2009. A notched-belly mutant with white-belly (DY1102) was identified after harvest of 2010 (M4 seeds). This mutant has high percentage of notched-belly grain, being 83.36% in 2011 (M5 seeds) and in 73.74% in 2012 (M6 seeds; Table 1). It is interesting that major part of the notched-belly grains have white-belly, which is visible on the fifth day after anthesis. This is obvious for the grains on the middle primary rachis of the panicle, which was used as the sampling position within panicle in this study (Table 1). Moreover, the white-belly only occurs in the bottom half part proximal to the embryo, i.e. below the notched line (Figure 1).
Table 1

Positional variation within panicle in ratios of white-belly grains to notched-belly grains in 2011 and 2012

Grain position

Notched-belly grain/total grain (%)

White-belly grain/notched-belly grain (%)

 

2011

2012

2011

2012

TPR

88.73

68.48

85.66

72.22

TSR

85.82

72.38

62.61

76.32

MPR

84.09

68.79

83.33

84.03

MSR

79.38

81.07

58.01

73.72

BPR

81.00

72.49

69.55

82.48

BSR

82.08

84.44

50.57

71.05

TWP

83.36

73.74

71.19

77.05

Note: TPR, Top primary rachis; TSR, top secondary rachis; MPR, middle primary rachis; MSR, middle secondary rachis; BPR, bottom primary rachis; BSR, bottom secondary rachis; TWP, the whole panicle.

Comparison system

Using DY1102, we developed a novel comparison system aiming to evaluate the effect of chalkiness on the protein expression. As shown in Figure 2, notched-belly grains without white-belly was used as the control. First, comparison between the bottom part (T2) and upper part (T1) can quantify the effect of embryo. Second, comparison of the bottom part (C2) and upper part (C1) of grain with white-belly can evaluate the compound effect of embryo and chalkiness. Thus, the effect of chalkiness can be measured through a further comparison between C2 vs C1 and T2 vs T1, by which the embryo effect was minimized. Importantly, these comparisons are made within the same grain, which has the identical genotype or genetic background, and thus are more efficient than those made between different grains within one panicle or from different varieties.
Figure 2

The experimental scheme of the sampling and iTRAQ analysis. C1 and C2, the upper and bottom half part of grain with white-belly, respectively. T1 and T2, the upper and bottom half part of grain without white-belly, respectively. Note that the embryos of C2 and T2 were removed.

SEM and amylopectin structure analysis

At maturity, grains from the middle primary rachis of the panicle were collected and then dehusked as brown rice. Typical notched-belly grains with and without white-belly were selected. After the embryo removed, grains were cut into two parts along the notched line, resulting in two kinds of samples for both grain types, i.e. T1 and T2 for the translucent grains and C1 and C2 for the grains with white-belly (Figure 2). For scanning electron microscope (SEM) analysis, samples were completely dried under low pressure and then were transversely cut with a razor blade, producing a fracture rather than a clean cut. The fracture was sputter-coated with gold in vacuum and observed by SEM (Hitachi S-3000 N) at an accelerating voltage of 15 kV.

Amylopectin of the four samples were extracted and purified using the alkaline-steeping method of Patindol et al.[11]. Amylopectin was debranched by isoamylase (I5284-5MU, Sigma-Aldrich) and then separated by high-performance size-exclusion chromatography, according to Yang et al.[12]. The degree of polymerization (DP) of the linear fractions in debranched amylopectin was calculated as their molecular weight divided by 162. The analyses were performed with three replications for each sample.

Protein extraction

Proteins of the four parts were extracted according to the method of Ding et al.[13]. Briefly, samples were grinded about 0.1 g were suspended with ice-cold 10% (w/v) trichloroacetic acid in acetone containing 10 mM dithiothreitol and 1 mM phenylmethylsulfonyl fluoride, and then incubated at −20°C for 1 h, followed by centrifugation at 20000 × g for 30 min at 4°C in a refrigerated high-speed centrifuge. The precipitate was washed three times by suspending in cold acetone. After vacuum drying, the precipitate (~40 mg) was dissolved in 1 ml 0.5 M triethylammonium bicarbonate buffer. Protein concentration was measured by the Bradford method using bovine serum albumin as the standard.

In-solution trypsin digestion and iTRAQ procedure

Trypsin digestion and iTRAQ analysis were performed by Beijing Genomics Institute. Total protein (~100 μg) of each sample was reduced by adding dithiothreitol to a final concentration of 10 mM and incubated for 1 h, then alkylated with 55 mM iodoacetamide for 1 h at room temperature. Samples were digested using sequencing grade trypsin solution (10 ng/μl in 25 mM ammonium bicarbonate) for 12 h at 37°C. After digestion, the peptide segment was freeze-dried in a centrifugal speed vacuum concentrator.

Two replications for each sample were performed for iTRAQ analysis. The peptide segment of each sample was labeled using iTRAQ 8-plex kits according to the manufacturer's manual (AB Sciex Inc., USA). As shown in Figure 2, two replications of T1 were labeled with reagent 113 and 117, T2 with reagent 114 and 118, C1 with reagent 115 and 119, and C2 with reagent 116 and 121, respectively. After labeling and quenching, samples were combined and lyophilized before redissolving in 4 ml of buffer A (25 mM NaH2PO4 in 25% acetonitrile, pH 2.7). Fractionation was conducted though the strong cation exchange chromatography on an Ultremex SCX column using HPLC (Shimadzu LC-20AB). The mixed sample was eluted with buffer A for 10 min, then eluted with a gradient of 5%-80% buffer B (25 mM NaH2PO4, 1 M KCl in 25% acetonitrile, pH2.7) for 12 min, at a flow rate of 1 ml/min. The process was monitored by absorbance at 214 nm simultaneously. The resulting 12 fractions were collected according to the peak area, and then were desalted with StrataX desalting column and lyophilized.

LC-MS/MS analysis

The system of UPLC (nanoACQuity, Waters) coupled with tandem mass spectrometry (TripleTOF 5600, AB SCIEX, Concord, ON) was used for peptides identification and quantification. The data acquisition was performed according to Wang et al.[14]. Briefly, a TripleTOF 5600 System fitted with a Nanospray III source and a pulled quartz tip as the emitter was used for tandem mass spectrometry. Data was acquired using an ion spray voltage of 2.5 kV. The MS was operated with TOF-MS scans. For information dependant acquisition, the MS survey scans were acquired in 250 ms and the top 30 product ion were selected for MS/MS scans.

Bioinformatics analysis

All MS/MS spectra were searched against in the NCBInr Oryza sativa sequence databases and UniProtKB/Swiss-Prot database with MASCOT software (Matrix Science, UK; version 2.3.02). For biological replications, spectra from the 12 fractions were combined into one file and searched. The search parameters were as follows: (1) allowing one missed cleavage in the protein trypsin digests; (2) fixed modifications of carbamidomethylation at Cys, variable modifications of oxidation at Met and iTRAQ 8-plex at Tyr; (3) peptide tolerance was set at ±0.1 Da and MS/MS tolerance was set at ±0.05 Da. The peptide charge was set as Mr, and monoisotopic mass was chosen. The iTRAQ 8-plex was chosen for quantification during the search.

The search results were filtered before data exportation. The filters were used for protein identification with these options: significance threshold P < 0.05 (with 95% confidence) and ion score or expected cutoff less than 0.05 (with 95% confidence). For protein quantitation, the filters were set as follows: (1) “median” was chosen for the protein ratio type; (2) the minimum precursor charge was set to 2 and minimum peptides were set to 2, and only unique peptides were used for quantitation; and (3) normalization by median intensities, and outliers were removed automatically. The peptide threshold was set as above for identity. A 1.2-fold change was set to identify significant differentially expressed proteins in addition with P-value < 0.05.

The differentially expressed proteins were classified using the Gene Ontology database and Kyoto Encyclopedia of Genes and Genomes database.

Results

Morphological and amylopectin structure of the chalky endosperm

SEM photos show the typical characteristic of the chalky tissues of the grains with white-belly (Figure 3). Starch granules are loosely packed in the opaque endosperm cells (Figure 3C), as compared with that of the translucent tissues of grains without white-belly or the translucent upper part of the grains with white-belly (Figure 3A). In addition, in comparison with that of the wild type (Figure 3B), chalky tissues of DY1102 are easily broken under the mechanical stress during sample preparation, indicating differences in chemical composition or microstructure of the chalky tissue between DY1102 and its wild type.
Figure 3

Scanning electron microscopy images of starch granule in DY1102 and WT (wide type). A, The translucent tissue of the upper half part (above the notched line) of grains with white-belly; B, The white-belly tissue of grains from wild type, Wuyujing3; C, The chalky tissue of the bottom half part (below the notched line) of grains with white-belly. Bars = 100 μm.

In this study, notched-belly grain without white-belly was used as the control. Adopting the above mentioned comparison system in the Methods section, the effect of chalkiness on starch fine structure can be evaluated by the comparison between C2 vs C1 and T2 vs T1. The result revealed that the chalky tissue contained more short chain (DP ≤ 12) and less medium and long chain as compared with the translucent tissue (Figure 4). This finding agrees with that of Liu et al.[5] and Patindol and Wang [15].
Figure 4

The chain-length distribution of amylopectin of the chalky and translucent parts grains with white-belly (C) and without white-belly (T).

Proteins identified by iTRAQ and their functional classification

Total proteins in the four samples (T1, T2, C1, and C2) were explored using the iTRAQ technique with two biological replications. Analysis of protein extracts from these samples resulted in the detection and identification of 1503 (4031 unique peptides; Additional file 1). The number of rice endosperm proteins identified in this study is larger than that using 2-DE, being about 500 spots by Li et al. [10] and 302 by Yang et al.[16]. It is greater than that obtained by multidimensional protein identification technology, being 822 proteins as reported by Koller et al.[17].

Proteins were considered as being differentially expressed according to Neilsen et al.[18], which have both a fold-change more than 20% and a p-value below 0.05. A total of 113 proteins showed differential expression by comparison between C1 vs C2 and T1 vs T2, i.e. the proteins responsible for chalkiness formation (Tables 2 and 3). Among them, 70 proteins were up-regulated and 43 down-regulated. According to Gene Ontology (GO) database, these proteins fell into 13 major categories. As shown in Figure 5, the most abundant category was classified as being involved in protein synthesis, folding and degradation (27.4% of the total differentially expressed proteins). The second most abundant class consisted of proteins with yet unidentified function or proteins with no detectable homology to other predicted proteins in the database (24.8% of the total differentially expressed proteins). The third abundant category belongs to carbohydrate metabolism, accounting for 15.0% of the total differentially expressed proteins. Furthermore, seven proteins associated with redox homeostasis have been detected.
Table 2

Functional classification of up-regulated proteins

Accession

Protein Name

Score

Mass (kDa)

Cov. (%)

Unique peptide

C2/C1

T2/T1

C/T

Amino acid metabolism

       

gi|385717668

5-methyltetrahydropteroyltriglutamate-homocysteine methyltransferase

768

100.7

12.1

7

0.322

0.260

1.238

gi|77548611

2-isopropylmalate synthase A

677

78.0

23

9

0.938

0.721

1.301

Carbohydrate metabolism

       

gi|78099751

Fructose-bisphosphate aldolase cytoplasmic isozyme

921

48.7

24

4

0.855

0.662

1.292

gi|113632010

Triosephosphate isomerase, chloroplastic

315

38.8

20.4

4

0.400

0.290

1.379

gi|113548195

Probable rhamnose biosynthetic enzyme 1

241

91.2

7.3

3

0.382

0.261

1.464

gi|40253646

putative starch synthase DULL1

155

231.2

3

5

1.451

0.990

1.466

gi|113580063

UDP-glucose 4-epimerase GEPI48

183

45.8

6.8

2

0.312

0.208

1.500

gi|113548194

UDP-glucuronic acid decarboxylase 1

220

46.1

14.6

3

0.566

0.340

1.665

gi|222628767

2-oxoglutarate dehydrogenase, mitochondrial

249

129.0

4.9

4

0.163

0.096

1.698

gi|113549799

UDP-glucose 6-dehydrogenase

188

65.0

11.9

3

0.173

0.081

2.136

gi|75327567

Probable cinnamyl alcohol dehydrogenase 6

92

46.0

4.2

1

0.437

0.135

3.237

gi|75133690

UDP-arabinopyranose mutase 3

243

49.9

16.7

5

0.270

0.074

3.649

gi|75156168

Hexokinase-1

152

56.2

4.6

2

0.333

0.054

6.167

Cell defense

        

gi|113533098

Heterogeneous nuclear ribonucleoprotein A2/B1-like

131

50.1

10.5

2

1.567

1.241

1.263

gi|113580000

Late embryogenesis abundant protein Lea14-A

63

20.4

7.3

1

1.528

1.128

1.355

gi|22711545

Putative cytochrome P450

58

120.8

0.9

1

0.088

0.051

1.725

gi|113649843

P21 protein, putative, expressed

269

29.3

21.8

5

1.632

0.824

1.981

gi|113649501

Pathogenesis-related protein 1

197

21.3

38.1

4

1.380

0.500

2.760

gi|113649505

Major pollen allergen Bet v 1-D/H

1402

21.5

75.3

10

1.814

0.567

3.199

Coenzyme metabolism

       

gi|54291831

C-1-tetrahydrofolate synthase, cytoplasmic

57

36.7

4.8

1

0.407

0.159

2.560

Energy production

       

gi|113548489

ATP-dependent transporter ycf16, putative, expressed

172

38.0

15.1

3

0.900

0.747

1.205

gi|75294330

Probable succinyl-CoA ligase [ADP-forming] subunit alpha, mitochondrial

205

41.3

12.1

3

0.998

0.645

1.547

gi|113535585

Putative vacuolar proton-ATPase

475

79.8

14

2

0.400

0.110

3.636

gi|113533574

Putative vacuolar ATPase B subunit

1023

60.4

30.9

9

0.304

0.082

3.707

Lipid metabolism

        

gi|113595159

Sterol carrier protein 2-like

210

18.4

28.7

3

1.084

0.820

1.322

gi|122248693

Non-specific lipid-transfer protein 3

241

14.1

24.8

2

1.598

1.122

1.424

Protein synthesis, folding and degradation

       

gi|113579500

Protein translation factor SUI1 homolog

63

16.8

11.3

1

0.977

0.797

1.226

gi|122246932

Cysteine proteinase inhibitor 8

216

13.5

36.6

2

1.247

0.995

1.253

gi|38605801

40S ribosomal protein S27

288

7.4

66.7

2

0.855

0.672

1.272

gi|125584147

Tubulin-specific chaperone A

67

17.2

8

1

1.801

1.404

1.283

gi|108711183

26S proteasome non-ATPase regulatory subunit 10, putative, expressed

259

29.4

25.4

4

0.936

0.719

1.302

gi|113535779

26S proteasome regulatory particle triple-A ATPase subunit 6

177

58.0

18.6

5

0.437

0.326

1.340

gi|1703380

ADP-ribosylation factor 2

336

24.4

35.4

5

0.623

0.463

1.346

gi|222641792

Heat shock protein 81-2

461

56.5

19.5

2

1.535

1.110

1.383

gi|113531460

Bowman-Birk type wound-induced proteinase inhibitor WIP1

167

15.2

10

1

1.353

0.946

1.430

gi|113649350

Eukaryotic translation initiation factor 5A-2

212

22.6

29.4

3

1.179

0.821

1.436

gi|730456

40S ribosomal protein S19

375

20.1

41.1

6

0.860

0.581

1.480

gi|391875

40S ribosomal protein S20

135

17.7

21.4

1

0.847

0.562

1.507

gi|113550094

T-complex protein 1 subunit theta

244

70.8

11.7

4

0.367

0.240

1.529

gi|14589381

Alanine--tRNA ligase

228

95.3

9.9

5

0.797

0.474

1.681

gi|122232855

Clathrin heavy chain 1

229

224.0

6

7

0.490

0.274

1.788

gi|62900360

Importin subunit alpha-1a

159

67.0

5.3

2

0.290

0.156

1.859

gi|255672966

Putative density regulated protein drp1

244

28.6

38.2

4

1.035

0.547

1.892

gi|122169274

Coatomer subunit delta-2

93

69.0

7.3

3

0.521

0.220

2.368

gi|113548306

40S ribosomal protein S7

90

28.9

16.1

2

0.450

0.173

2.601

gi|75325389

Eukaryotic initiation factor 4A-3

428

53.5

25.1

8

0.514

0.173

2.971

gi|38347158

Chaperone protein ClpC1, chloroplastic

294

116.5

12.5

6

0.986

0.295

3.342

Redox homeostasis

       

gi|122166938

Peroxidase 2

172

35.5

13.1

3

1.418

1.045

1.357

Secondary metabolites biosynthesis

       

gi|75261413

4-hydroxy-3-methylbut-2-en-1-yl diphosphate synthase, chloroplastic

180

93.3

6

3

0.167

0.027

6.185

Signal transduction

       

gi|122235035

Calmodulin-3

276

20.2

22.8

1

1.310

1.083

1.210

gi|75323484

Calmodulin-2

510

20.5

22.8

1

1.434

1.180

1.215

gi|113532001

Ras-related protein Rab7

136

28.0

16.9

3

0.692

0.390

1.774

Transcription

        

gi|113622935

Putative quinone-oxidoreductase QR2

199

26.1

25.1

4

0.625

0.478

1.308

Transport

        

gi|113639089

Protein CutA1, chloroplastic

348

21.6

22.9

3

1.327

1.045

1.270

gi|113649744

Sulfurtransferase

461

47.3

32.8

8

0.977

0.680

1.437

gi|113578690

ADP, ATP carrier protein 1, mitochondrial

197

50.6

9.2

3

0.502

0.137

3.664

Unknown pathway

       

gi|113549649

hypothetical protein

166

12.0

17.4

2

1.777

1.423

1.249

gi|113579243

Pleckstrin homology domain-containing protein 1

129

21.9

7

1

0.916

0.728

1.258

gi|113596594

Os06g0711900

105

17.7

11.2

1

1.618

1.267

1.277

gi|3492928

16 kDa oleosin isoform R16

131

17.7

6.1

1

1.363

1.031

1.322

gi|113623942

Os08g0459300

204

27.3

29.2

3

1.222

0.920

1.328

gi|113596416

Putative phytocyanin protein, PUP2

158

28.4

12.2

3

1.217

0.908

1.340

gi|113532536

Outer-envelope membrane of Chloroplasts 34-like

425

747.7

2.5

10

1.210

0.871

1.389

gi|77550956

EF hand family protein

164

12.1

10.4

1

1.423

1.021

1.394

gi|75106519

Early nodulin-like protein 1

512

26.8

12.7

2

1.577

1.096

1.439

gi|53792234

Bowman-Birk type bran trypsin inhibitor

77

33.2

4.5

1

1.109

0.752

1.475

gi|46981317

unknown protein

70

60.7

4.5

2

0.636

0.380

1.674

gi|113547324

Gamma-thionin PPT, putative, expressed

573

10.7

27.2

2

1.552

0.920

1.687

gi|113623527

Os08g0327700 (Putative seed maturation protein)

224

17.6

13.3

1

1.792

0.965

1.857

gi|113578614

Putative pentatricopeptide repeat-containing protein At1g10330

51

58.4

1.4

1

1.884

0.516

3.651

Note: Notched-belly grain without white-belly was used as the control. The effect of embryo was quantified by comparison between the bottom part (T2) and upper part (T1). Comparison of the bottom part (C2) and upper part (C1) of grain with white-belly indicated the compound effect of embryo and chalkiness. Therefore, the effect of chalkiness can be evaluated through a further comparison between C2 vs C1 and T2 vs T1, by which the embryo effect was eliminated. Cov. , average percentage of assigned peptides to the predicted protein.

Table 3

Functional classification of down-regulated proteins

Accession

Protein Name

Score

Mass (kDa)

Cov. (%)

Unique peptide

C2/C1

T2/T1

C/T

Amino acid metabolism

       

gi|584706

Aspartate aminotransferase, cytoplasmic

320

49.8

15.7

6

0.788

1.150

0.685

gi|113535557

Putative glycine decarboxylase complex H-protein

117

20.8

15.2

2

1.055

1.308

0.807

Carbohydrate metabolism

       

gi|222640045

Putative aconitate hydratase, cytoplasmic

926

120.0

9.6

6

0.208

0.821

0.253

gi|28190676

Transketolase, chloroplastic

221

92.7

9.2

4

0.065

0.137

0.474

gi|113534863

Putative xylanase inhibitor

123

49.4

8.8

3

0.637

0.872

0.731

gi|108885236

Glucose and ribitol dehydrogenase homolog

276

37.3

23.7

6

1.015

1.288

0.788

gi|75114635

Probable alpha-glucosidase

676

102.6

5.1

4

1.135

1.364

0.832

gi|108707955

2,3-bisphosphoglycerate-independent phosphoglycerate mutase (PGAM)

261

72.8

6.1

1

0.040

-

-

Cell defense

        

gi|75298023

17.9 kDa class I heat shock protein

301

22.5

17.4

2

1.147

1.756

0.653

gi|1169521

Embryonic abundant protein 1

151

12.3

35.8

3

1.792

2.271

0.789

gi|113648660

Os12g0147200

327

19.1

32

3

1.048

1.299

0.807

Energy production

       

gi|113537902

Cytochrome b5 domain-containing protein-like

279

13.3

55.9

4

1.207

1.786

0.676

Lipid metabolism

       

gi|113623031

Acyl-CoA-binding protein

200

13.5

54.9

2

1.660

2.026

0.819

Protein synthesis, folding and degradation

       

gi|113549785

60S ribosomal protein L13a-4

85

31.1

6.3

1

0.541

1.081

0.500

gi|113624448

Cysteine proteinase 3 (Fragment)

182

48.9

13

3

1.177

1.663

0.708

gi|548770

60S ribosomal protein L3

64

61.3

6.7

2

0.169

0.238

0.710

gi|113649731

Ubiquitin-conjugating enzyme E2 variant 1C

238

19.5

29.5

2

0.734

1.031

0.712

gi|113535206

Dnak-type molecular chaperone Bip

4150

92.7

42.7

21

0.696

0.961

0.724

gi|556560

26S protease regulatory subunit 6A homolog

413

58.0

16.6

4

0.500

0.690

0.725

gi|113535132

RuBisCO large subunit-binding protein subunit beta, chloroplastic (Fragment)

791

80.6

20.1

4

0.566

0.777

0.728

gi|222642001

Putative UIP2 (SKP1-like 2, UFO-binding protein 2)

153

23.7

27.4

2

0.423

0.545

0.776

gi|75322635

Protein disulfide isomerase-like 2-3

289

60.2

15.6

5

0.817

1.018

0.803

gi|113579164

Luminal-binding protein 2/B-70/Bip 2

454

86.3

4.1

3

0.579

0.718

0.806

Redox homeostasis

       

gi|113579377

Aldose reductase

222

44.4

27.7

6

1.183

1.575

0.751

gi|113550330

Putative oxidoreductase

97

42.0

9.9

2

0.789

1.030

0.766

gi|52076516

Thioredoxin O, mitochondrial

65

24.5

14.3

2

0.508

0.629

0.808

gi|516839

Catalase isozyme B

319

64.3

22.2

5

0.719

0.878

0.819

gi|119370643

Glutaredoxin-C8

398

18.8

44.9

6

0.680

0.824

0.825

gi|29367419

Peptide methionine sulfoxide reductase B5

265

21.3

29.8

3

1.188

1.437

0.827

Unknown pathway

       

gi|284431762

Prolamin PROL 17D

356

18.6

35.9

1

0.435

1.319

0.330

gi|62733566

Os03g0723400

335

14.3

70.9

3

0.581

1.683

0.345

gi|306415963

Glycine-rich RNA-binding protein 1 (Fragment)

2043

17.0

41

1

0.496

1.351

0.367

gi|122222504

Protein SGT1 homolog

302

52.6

7.1

2

0.512

1.148

0.446

gi|113624371

Os08g0543600

98

104.8

3.7

2

0.625

1.182

0.529

gi|113536747

Os02g0576400

123

14.0

26.9

2

0.886

1.655

0.535

gi|113537457

Os02g0715400

298

11.9

32.7

2

0.848

1.440

0.589

gi|28564794

Putative uncharacterized protein P0534A03.117

258

25.8

24.4

3

0.792

1.342

0.590

gi|255672911

Vegetative cell wall protein gp1-like

108

66.4

8.1

3

0.979

1.430

0.685

gi|113578822

Ran-binding protein 3

82

63.4

4.9

2

1.220

1.719

0.710

gi|77556700

Os12g0626500

1606

16.3

38.6

3

1.019

1.396

0.730

gi|113537680

Annexin D7

144

42.1

13.4

4

0.747

0.951

0.785

gi|113533811

Putative calcium-binding protein

245

72.6

8.6

4

1.015

1.290

0.787

gi|18652814

Zinc finger protein ZAT7

102

19.7

8.8

1

1.165

1.420

0.820

Note: “-”, not detected.

Figure 5

Functional classification and distribution of the differentially expressed proteins via the Gene Ontology (GO) database. A, Total differentially expressed proteins(113); B, Up-regulated proteins (70); C, Down-regulated proteins (43).

In summary, we identified 113 proteins responsible for grain chalkiness formation. Of these, 52.1% proteins involve in carbohydrate metabolism, nitrogen metabolism including amino acid biosynthesis and protein synthesis, assembly, and degradation, and redox homeostasis.

Proteins associated with carbohydrate metabolism

Seventeen differentially expressed proteins associated with carbohydrate metabolism were identified. These proteins were metabolic enzymes directly involved in starch synthesis and hydrolysis, cell wall biogenesis, glycolysis, pentose phosphate pathway and TCA cycle. As shown in Figure 6, most of the enzymes identified are up-regulated, except for three enzymes in the TCA cycle (aconitate hydratase), pentose phosphate pathway (transketolase), and starch hydrolysis (α-glucosidase).
Figure 6

Overview of differentially expressed proteins onto carbohydrate metabolism associated with rice grain chalkiness. Up-regulated proteins are designated in red font and down-regulated proteins are designated in green font. ACO, aconitate hydratase; AGH, alpha-glucosidase; Araf, arabinofuranose; Arap, arabinopyranose; DULL1, putative starch synthase DULL1; FBA, fructose-bisphosphate aldolase; Frc, fructose; GA-3P, glyceradehycle 3-phosphate; Gal, galactose; GalA, galacturonic acid; Gdl, gluconolactone; Glc, glucose; GlcA, glucuronic acid; HXK, hexokinase; OAA, oxaloacetate; ODH, 2-oxoglutarate dehydrogenase; P, phosphate; PEP, phosphoenolpyruvate; PGAM-i, 2,3-bisphosphoglycerate independent phosphoglycerate mutase; RHM, rhamnose biosynthetic enzyme; Rha, rhmannose; Ru-5P, ribulose 5-phosphate; TK, transketolase; TPI, triosephosphate isomerase; UAM, UDP-arabinopyranose mutase; UGD, UDP-glucose 6-dehydrogenase; UGE, UDP-glucose 4-epimerase; UXS, UDP-glucuronic acid decarboxylase; Xyl, xylose; 2-OG, 2-oxoglutarate; 2-PGA, 2-phosphoglycerate; 3-PGA, 3-phosphoglycerate.

Notably, proteins involved in starch accumulation were promoted. The enzyme Dull1, which is responsible for the synthesis of long chain of amylopectin, was up-regulated. By contrast, the α-Glucosidase involved in starch hydrolysis was down-regulated. In addition, we identified five up-regulated enzymes related to cell wall synthesis, including rhamnose biosynthetic enzyme, UDP-glucose 4-epimerase, UDP-glucose 6-dehydrogenase, UDP-arabinopyranose mutase, and UDP-glucuronic acid decarboxylase. This finding indicates the potential role of cell wall synthesis in the formation of endosperm chalkiness.

Proteins involved in protein synthesis, assembly and degradation

We obtained 31 proteins related to protein synthesis, folding and degradation (Figure 7). For protein synthesis, basic components of ribosome, mainly the 60S ribosomal proteins (L3 and L13a-4) were identified as being down-regulated, whereas 40S ribosomal proteins (S7, S19, S20, and S27) were identified as being up-regulated. In addition, eIF 4A-3 and eIF 5A-2 proteins were up-regulated. Four molecular chaperones were found to be down-regulated in the endoplasmic reticulum, including BiP1 (dnak-type molecular chaperone BiP), BiP2 (luminal-binding protein 2), PDIL 2–3 (protein disulfide isomerase-like 2–3), and Hsp40 (dnaJ homolog subfamily B member 11). Six proteins were identified in the ubiquitin/26S proteasome system, the major location for protein degradation. Among these proteins, the RPN10, RPT6, and Hsp 90 were up-regulated. However, the ubiquitin-conjugating enzyme E2, Skp1, and RPT5a were down-regulated. Previous studies showed that, knockout of PDIL genes like PDIL 1–1 can result in grain chalkiness [19], and mutant with over-expressed or knockdown of BiP genes displayed an opaque phenotype [7]. Thus the down-regulation of PDIL 2–3 and BiP proteins identified in this study could be responsible for the occurrence of endosperm chalkiness.
Figure 7

Differentially expressed proteins associated with protein synthesis, folding, and degradation. Up-regulated proteins are designated in red font and down-regulated proteins are designated in green font. BiP, dnak-type molecular chaperone BiP and Luminal-binding protein 2; Hsp, heat shock protein; PDI, protein disulfide isomerase like 2–3; RPN10, 26S proteasome non-ATPase regulatory subunit 10; RPT5a, 26S protease regulatory subunit 6A homolog; Skp1, putative UIP2 ( SKP1-like); RPT6, 26S proteasome regulatory particle triple-A ATPase subunit 6.

Proteins related to redox homeostasis

The Asc/GSH cycle, consisting of glutathione, ascorbic acid and related metabolic enzymes, is an important part of ROS scavenging mechanism to reduced peroxides [20]. Liu et al.[5] reported that an imbalance in ROS concentrations in endosperm may contribute to the development of grain chalkiness, and glutathione-S-transferase, glyoxalase, lipoxygenase-5, and thioredoxin (TRX) were responsible for maintaining the homeostasis of ROS. We found four proteins involved in the ROS-scavenging mechanism of rice chalky endosperm (Figure 8). Among these, catalase isozyme B, thioredoxin O, glutaredoxin-C8 were down-regulated, whereas peroxidase 2 were up-regulated. Our findings agree with those of Liu et al.[5], suggesting a close relation between redox homeostasis and grain chalkiness.
Figure 8

Differentially expressed proteins involved in ROS-scavenging mechanism. Up-regulated proteins are designated in red font and down-regulated proteins are designated in green font. Asc, ascorbate; APX, ascorbate peroxidase; CAT, catalase; DHA, dehydroascrobate; MDA, monodehydroascorbate; GLU, glutaredoxin; GPX, glutathione peroxidase; GSH, reduced glutathione; GSSG, oxidized glutathione; ROS, reactive oxygen species; TRX, thioredoxin; Prx, peroxidase.

Additional proteins related to grain chalkiness

In addition to proteins involved in carbon and nitrogen metabolism, and redox homeostasis, proteins of five additional metabolic processes should be mentioned. (1) proteins associated with inorganic ion transport like protein CutA1 and sulfurtransferase. (2) signal transduction related proteins, such as calmodulin-2 and calmodulin-2 that mediates the control of a large number of enzymes, ion channels, and other proteins by Ca2+. (3) proteins involved in cell defense, such as late embryogenesis abundant protein Lea14-A, pathogenesis-related protein, and major pollen allergen Bet v 1-D/H. (4) the seed storage protein prolamin PPROL 17D. (5) proteins involved in other metabolisms except carbon and nitrogen, including lipid metabolism (non-specific lipid-transfer protein and Acyl-CoA-binding protein), coenzyme metabolism (C-1-tetrahydrofolate synthase), and secondary metabolites biosynthesis (4-hydroxy-3-methylbut-2-en-1-yl diphosphate synthase). Collectively, our results indicate that the formation of grain chalkiness is associated with diverse biological processes and multiple genetic pathways.

Discussion

The practical value of the comparison system based on the notched-belly mutant with white-belly

Grain chalkiness has been the major objective of rice breeding and cultivation. It is a rather complicated trait controlled both by genetic and environmental factors. Up to now, genomic, transcriptional, and proteomic approaches have been adopted to explore the genes or biochemical pathways responsible for chalkiness formation, by which our knowledge of grain chalkiness has been broadened [5, 9, 21]. Nevertheless, only few QTLs or genes have been identified and functionally analyzed. The molecular mechanisms of endosperm chalkiness are still imperfectly understood.

Proteomic method has been employed to elucidate the physiological foundation of grain chalkiness, and the effect of high temperature has been investigated extensively [9, 10]. However, comparisons of protein expression in these studies were conducted either between varieties or between chalky grains and perfect grains for a given variety. These comparisons have limitations that it can not avoid the effect of genotype for grains between varieties and the effect of growing environment for grains of the same variety. Even if they are from the same panicle, the different position means different flowering date, which results in different meteorological conditions for grain filling.

We identified a notched-belly mutant with white-belly (DY1102) in 2010. This mutant has high percentage of notched-belly grain. The notched line is visible on the fifth day after anthesis, which enable us chasing the process of chalky tissue formation. Notably, the white-belly only occurs in the bottom part proximal to the embryo, with the upper half part being translucent. In addition, about 15% of the notched-belly grains do not have white-belly, which can be used as the control for comparisons. Using this mutant, we developed a novel comparison system, and thereby enzymes or biochemical pathways responsible for chalkiness formation were identified, including pathways of carbohydrate metabolism, protein synthesis, folding, and degradation, and ROS scavenging. These pathways confirmed the previous findings by other researches [5, 8, 9], and should be further examined in future studies on grain chalkiness.

It should be noted that some results of this study are contrary to previous studies, which may be associated with the materials used. Take cell wall synthesis as an example. Liu et al.[5] made a transcriptional comparison between a near-isogenic line CSSL50-1 with high chalkiness and its normal parental line Asominori for grain endosperm chalkiness. Their results showed that the enhancement of sucrose and starch synthesis in grains of CSSL 50–1 is at the cost of cell wall related nonstorage polysaccharides, suggesting the possible role of the disorders in carbohydrate metabolism in the formation of endosperm chalkiness. By contrast, our results revealed the promotion of starch synthesis is accompanied by the increased expressions of five enzymes involved in cell wall synthesis (Table 2). Interestingly, this result was obtained by comparisons between T1 vs T2 and C1 vs C2, using grains without white-belly as control, by which the effect of embryo was evaluated. However, if this control is not used, the comparison between C1 and C2 would result in an opposite conclusion that the five proteins were down-regulated in the chalky tissue. This example highlights the high value of DY1102-based comparison system to exploring the underlying mechanism of chalkiness formation.

Carbon metabolism in relation to grain chalkiness

Starch synthesis

Amylopectin makes up 65–85% of starch weight. The major starch synthase (SS) isozymes responsible for amylopectin biosynthesis in rice endosperm are SSI, SSIIa, and SSIIIa. SSI generates chains with a DP 8–12 from short DP 6–7 chains [22]. By contrast, SSIIIa elongates the amylopectin B2–4 chains with DP >30 [23]. Proteomic analysis of this study showed that DULL1 (SSIIIa) was up-regulated. However, the increased expression of DULL1 did not cause increase in the ratio of long chains. As revealed by the results of HPSEC, in comparison with the translucent parts, the chalky part contained more short chain (DP ≤ 12) and less medium and long chain. Fujita et al.[24] reported that SSI or SSIIIa is indispensable for starch biosynthesis in rice endosperm, and these isozymes can strongly compensate for each other when the counterpart is lacking. Thus it is still unknown whether the increased level of short chain is the result of compensation from other SSs like SSI or not, which needs further investigation.

Cell wall synthesis

Cell walls make up a major part of the dry weight of plants, and at times of rapid growth, their synthesis may be a major drain on the resources of the cell, accounting for 30% or more of cellular carbohydrate metabolism. Five enzymes responsible for cell wall synthesis, including rhamnose biosynthetic enzyme, UDP-glucose 4-epimerase, UDP-glucose 6-dehydrogenase, UDP-arabinopyranose mutase, and UDP-glucuronic acid decarboxylase, were detected in this study. In addition, the five proteins were all up-regulated in the chalky endosperm of grains with white-belly. This finding disagrees with that of Liu et al.[5], which showed down-regulation of genes responsible for cell wall synthesis (two cellulose synthase genes) and up-regulation of genes for cell wall hydrolysis (α-L-arabinofuranosidase and α-D-xylosidase). This is partially due to the differences in: (1) materials used, as mentioned above; and (2) methodology employed between proteomics and transcriptome [5]. Nevertheless, the two studies collectively indicate the significance of the cell wall synthesis for the elucidation of chalkiness formation.

Starch degradation

In addition to starch synthesis, there is growing awareness of the role of starch hydrolysis in the occurrence of grain chalkiness. The following evidences support this: (1) SEM photos showed that many micro-pores occur on the surface of the compound granules. The pores are viewed as the evidence of α-amylase attack, indicating the involvement of starch-degrading enzymes in grain chalkiness [25, 26]. (2) The level of glucose in opaque endosperm was markedly high as compared with the corresponding translucent parts of perfect grains, indicating that amylolytic enzymes exist and work in the opaque parts of chalky grains [27]. (3) The mRNA expression of Amy1A, Amy1C, Amy3D, and Amy3E genes, as well as α-amylase activity, increased under high temperature stress, suggesting a relation of starch degradation by high-temperature induced α-amylase to the formation of grain chalkiness [28, 29]. α-Glucosidase degrades the product of α-amylase and β-amylase, maltose, short chain glucans, and maltosaccharides or limit dextrins, to glucose. Our proteomic analysis showed that it was down-regulated in the chalky part, confirming the relation between starch hydrolysis and chalkiness formation.

On the other hand, Ishimaru et al.[30] reported that the α-amylase mRNA was not detected in the chalky tissues during grain filling, suggesting that starch degradation by α-amylase not be the cause of the formation of chalky grain. However, these authors argued that the formation of chalkiness through the starch degradation α-amylase may have occurred at the later stage [30]. In this study, aldose reductase (AR) was identified as being down-regulated in the chalky tissue. It catalyzes D-glucose converted to D-sorbitol, and serves a functional role in the desiccation tolerance processes at late stage of grain filling [31]. Therefore, temporal expression pattern of proteins should be fully investigated in order to evaluate individual contribution of starch degrading enzymes or late expressed proteins like AR to chalkiness formation.

Role of protein accumulation in grain chalkiness formation

Proteins account for about 8% of the rice endosperm’s weight, filling the space between starch granules. The role of proteins in the formation of grain chalkiness has gained increasing awareness. For example, results of Lin et al.[9] suggested the relation between protein (small heat shock proteins) accumulation and chalkiness formation under high temperature. In this study, we found that proteins belonging to protein folding and degradation were differentially expressed between the chalky and translucent part of the notched-belly grains, indicating the important role of proteins in grain chalkiness formation.

Protein folding

Protein must fold into a precise three dimensional structure to carry out their biological function, which is regulated by a group of proteins referred to as molecular chaperones. Chaperones fall into two major groups. The first group, the Hsp70 family such as BiP1 and BiP2 maintains polypeptides in an unfolded state. The second family is the chaperonins, including protein disulfide isomerase (PDI), promote proper polypeptide folding. There is evidence that changes in BiP protein levels induce ER stress, and BiP overexpression results in an opaque phenotype in the whole endosperm of rice [32]. PDI-like (PDIL) proteins are members of a multigene family belonging to the thioredoxin (TRX) superfamily [19]. The failure to express PDIL genes results in a floury endosperm and an endoplasmic reticulum stress response in rice. Han et al.[21] reported a mutant T3612 with a deletion in a gene encoding a protein disulphide isomerase-like enzyme (PDIL1-1) produces small grains with a floury endosperm. In addition, the absence of PDIL1-1 is associated with endoplasmic reticulum stress in the endosperm, which is likely to underlie the formation of the floury endosperm in the mutant. In this study, down-regulation of molecular chaperones including BiP1, BiP2, and PDIL2-3 were detected in the chalky tissues, confirming the relation between protein folding and chalkiness formation. In review of findings of other studies which indicate a strong correlation between the expression of PDIL and BiP and grain chalkiness formation, we suggest that these chaperones should be emphasized in the studies on chalky formation.

Protein degradation

Protein degradation plays many important physiological role in the cell, removing abnormal proteins, facilitating the recycling of amino acids, and regulating protein activity by eliminating molecules that are no longer needed. One major proteolytic pathway in eukaryotes involves the Ubiquitin/26S Proteasome System that utilizes the post-translational modification of proteins by ubiquitin. The conjugation of ubiquitin to a protein is carried out by a ubiquinating enzyme complex, consisting of a ubiquitin-activating enzyme (E1), ubiquitin-conjugating enzyme (E2), and a ubiquitin-ligating enzyme (E3). Among them, E3 and E2 are considered to play a crucial role in the specificity of ubiquitination. Six proteins were detected in the ubiquitin/26S proteasome system, with Skp1 (E3) and E2 being down-regulated, indicating the involvement of protein degradation in the grain chalkiness. In addition, Zhang et al.[33] reported that mutants in OsVPS22 gene responsible for ubiquitin-mediated degradation of membrane proteins had a chalky endosperm in the grain, supporting the hypothesis that protein degradation has implication in grain chalkiness formation.

The importance of balance between C and N metabolism in future studies on grain chalkiness

So far, the majority of studies with respect to grain chalkiness have been focused on starch, relating its accumulation or degradation to the formation of chalky tissue [28, 34]. Our previous work showed that the insufficient accumulation of protein bodies that do not completely fill the air spaces between starch granules may be an explanation for chalkiness occurrence, as was also reported by Del Rosario et al.[35]. Therefore, both starch and proteins are equally important for the formation of grain chalkiness.

In rice grain, starch and protein are the products of carbon (C) and nitrogen (N) metabolism. During the rice seed development, sugars and amino acids transported from source organs are allocated to C and N metabolism to produce starch and proteins in precise quantities and ratios, which requires coordinated expression profiles of genes involved in synthesis of starch and storage [36]. Disorder or breakdown of the balances between C and N may be the possible causes of chalkiness formation.

So far, the mechanism by which plants receive and transduce signals relating to their C and N status and subsequently regulating C and N metabolism remains unresolved. In the future studies on grain chalkiness, more attention should be paid to three enzymes, which perform regulating function in grain C and N metabolism. (1) Hexokinase (HXK). Recent studies in plants have unveiled sugar sensing and signaling systems mediated by hexokinase as a glucose sensor in a hexokinase-independent way [37]. (2) Aspartate aminotransferase (AAT). It catalyzes the reversible transfer of the amino group from aspartate to α-ketoglutarate, yielding oxaloacetate and glutamate. The ability of AAT to interconvert these important C and N compounds places it in a key position to regenerate plant metabolism. For example, using enzymes including AAT and AS, plants direct assimilated nitrogen into inert asparagines, which has a higher N: C ratio than glutamine and therefore can transport and store nitrogen more efficiently when carbon skeletons are limiting. (3) Thioredoxin (TRX). It was reported that TRX h targets at proteins involved in C and N metabolism, like sucrose synthase, phosphoglycerate kinase, alanine aminotransferase, and BiP. Increased TRX h expression resulted in aberrant phenotypes, such as chalky and shriveled features of rice grains under high temperature [38]. This is partially associated with the breakdown of the balance between C and N metabolism, leading to the abnormal biosynthesis of storage materials.

In this study, the above three proteins, HXK1, AAT, and TRX were detected to be differentially expressed between the chalky endosperm and its counterpart translucent endosperm. An extensive investigation of proteins or genes regulating C and N metabolism, in particular HXK1, AAT, and TRX, should extend our knowledge of the mechanisms with respect to chalkiness formation.

Conclusions

Using iTRAQ and the novel comparison system, we compared the chalky part with the translucent part of a notched-belly mutant with white-belly. Consistent with previous studies, our comparative proteomic analysis reveals immense complexity of the mechanism underlying rice grain chalkiness. Notably, nearly half of the identified proteins are involved in several central metabolic or regulatory pathways including carbohydrate metabolism, protein synthesis, folding and degradation, and ROS metabolism. However, key proteins of interest, in particular those involved in cell wall synthesis and protein folding, need to be confirmed using other methods like Western blotting. This study provides a valuable proteomic resource for the characterization of grain quality pathways at molecular and biochemical levels. Further refining of DY1102 as genetic material will help eventually clone and engineer the major genes related to the occurrence of rice grain chalkiness.

Availability of supporting data

The mass spectrometry proteomics data have been deposited to the ProteomeXchange Consortium [1] via the PRIDE partner repository with the dataset identifier PXD001030.

Abbreviations

AAT: 

Aspartate aminotransferase

AR: 

Aldose reductase

AS: 

Asparagine synthetase

BiP: 

Binding protein

DP: 

Degree of polymerization

EMS: 

Ethyl methane sulfonate

FBA: 

Fructose-1, 6-bisphosphate aldose

GO: 

Gene Ontology

HPLC: 

High performance liquid chromatography

HPSEC: 

High performance size exclusion chromatography

HSP: 

Heat shock protein

HXK: 

Hexokinase

iTRAQ: 

isobaric tags for relative and absolute quantification

LC-MS/MS: 

High-performance liquid chromatography with tandem mass spectrometry

PDI: 

Protein disulphide isomerase

PDIL: 

Protein disulphide isomerase-like

PPDK: 

Pyruvate orthophosphate dikinase

QTLs: 

Quantitative trait loci

ROS: 

Reactive oxygen species

SEM: 

Scanning electron microscope

sHSP: 

small heat shock protein

TPI: 

Triose-phosphate isomerase

TRX: 

thioredoxin

UPLC: 

Ultra performance liquid chromatography.

Declarations

Acknowledgements

This work was supported in part by grants from the National Natural Science Foundation (31171485), the National High Technology Research and Development Program of China (2014AA10A605), and the National Science and Technology Supporting Program (2012BAD04B08).

Authors’ Affiliations

(1)
College of Agronomy, Nanjing Agricultural University/Key Laboratory of Crop Physiology Ecology and Production Management, Ministry of Agriculture
(2)
Jiangsu Collaborative Innovation Center for Modern Crop Production

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