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Molecular Characterization and Expression Profiling of the Protein Disulfide Isomerase Gene Family in Brachypodium distachyon L

  • Chong Zhu ,

    Contributed equally to this work with: Chong Zhu, Nana Luo, Miao He, Guanxing Chen

    Affiliation College of Life Science, Capital Normal University, Beijing, China

  • Nana Luo ,

    Contributed equally to this work with: Chong Zhu, Nana Luo, Miao He, Guanxing Chen

    Affiliation College of Life Science, Capital Normal University, Beijing, China

  • Miao He ,

    Contributed equally to this work with: Chong Zhu, Nana Luo, Miao He, Guanxing Chen

    Affiliation College of Life Science, Capital Normal University, Beijing, China

  • Guanxing Chen ,

    Contributed equally to this work with: Chong Zhu, Nana Luo, Miao He, Guanxing Chen

    Affiliation College of Life Science, Capital Normal University, Beijing, China

  • Jiantang Zhu,

    Affiliation College of Life Science, Capital Normal University, Beijing, China

  • Guangjun Yin,

    Affiliation College of Life Science, Capital Normal University, Beijing, China

  • Xiaohui Li,

    Affiliation College of Life Science, Capital Normal University, Beijing, China

  • Yingkao Hu ,

    yingkaohu@sohu.com (YH); yanym@cnu.edu.cn (YY)

    Affiliation College of Life Science, Capital Normal University, Beijing, China

  • Jiarui Li,

    Affiliation Department of Plant Pathology, Kansas State University, Manhattan, Kansas, United States of America

  • Yueming Yan

    yingkaohu@sohu.com (YH); yanym@cnu.edu.cn (YY)

    Affiliation College of Life Science, Capital Normal University, Beijing, China

Molecular Characterization and Expression Profiling of the Protein Disulfide Isomerase Gene Family in Brachypodium distachyon L

  • Chong Zhu, 
  • Nana Luo, 
  • Miao He, 
  • Guanxing Chen, 
  • Jiantang Zhu, 
  • Guangjun Yin, 
  • Xiaohui Li, 
  • Yingkao Hu, 
  • Jiarui Li, 
  • Yueming Yan
PLOS
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Abstract

Protein disulfide isomerases (PDI) are involved in catalyzing protein disulfide bonding and isomerization in the endoplasmic reticulum and functions as a chaperone to inhibit the aggregation of misfolded proteins. Brachypodium distachyon is a widely used model plant for temperate grass species such as wheat and barley. In this work, we report the first molecular characterization, phylogenies, and expression profiles of PDI and PDI-like (PDIL) genes in B. distachyon in different tissues under various abiotic stresses. Eleven PDI and PDIL genes in the B. distachyon genome by in silico identification were evenly distributed across all five chromosomes. The plant PDI family has three conserved motifs that are involved in catalyzing protein disulfide bonding and isomerization, but a different exon/intron structural organization showed a high degree of structural differentiation. Two pairs of genes (BdPDIL4-1 and BdPDIL4-2; BdPDIL7-1 and BdPDIL7-2) contained segmental duplications, indicating each pair originated from one progenitor. Promoter analysis showed that Brachypodium PDI family members contained important cis-acting regulatory elements involved in seed storage protein synthesis and diverse stress response. All Brachypodium PDI genes investigated were ubiquitously expressed in different organs, but differentiation in expression levels among different genes and organs was clear. BdPDIL1-1 and BdPDIL5-1 were expressed abundantly in developing grains, suggesting that they have important roles in synthesis and accumulation of seed storage proteins. Diverse treatments (drought, salt, ABA, and H2O2) induced up- and down-regulated expression of Brachypodium PDI genes in seedling leaves. Interestingly, BdPDIL1-1 displayed significantly up-regulated expression following all abiotic stress treatments, indicating that it could be involved in multiple stress responses. Our results provide new insights into the structural and functional characteristics of the plant PDI gene family.

Introduction

Three types of aid proteins are found in the endoplasmic reticulum (ER): peptidyl-prolylcis-transisomerase (PPI), protein disulfide isomerase (PDI), and molecular chaperone binding protein (BiP, also called calnexin/calreticulin proteins). These proteins play a dominant role in assisting nascent polypeptides in folding to form specific three-dimensional conformation of functional proteins by rate-limiting isomerization steps [1][3]. Various PDIs function in catalyzing, isomerizing, and reducing/oxidizing the formation of both intra-chain and inter-chain disulfide bonds. This non-specific binding of peptides that assists correct folding is viewed as a chaperone activity and includes calnexin/calreticulin proteins and BiP, but understanding the detailed molecular mechanisms require more in-depth research [4], [5]. PDIs are also the beta-subunit of human prolyl 4-hydroxylase and a component of the microsomal triglyceride transfer protein complex in mammalian cells [6], [7]. The PDI gene family encodes several PDI and PDI-like (PDIL) proteins and is a member of the thioredoxin superfamily that includes glutaredoxins, thioredoxins, ferredoxins, and peroxidoxins [8].

Typical well-known PDIs are composed of two approximately 57 kDa subunits of about 510 amino acids in length and are present in most eukaryotic species [9]. Molecular structures show that PDI family proteins have five discrete domains: a, b, b′, a′, and c [10]. The a and a′ domains have high sequence similarity to thioredoxin, and each contains an active -Cys-Gly-His-Cys- motif embraced by the sequence structures of α-helices and β-strands (β-α-β-α-β-α-β-β-α) that are essential for polypeptide redox and isomerization [11]. The b and b′ domains have low similarity, and the b′ domain provides the principal substrate binding site during isomerisation reactions, but the b domain plays only a structural role without catalytic activity [12]. The C-terminal has a high-capacity Ca2+-binding site and ends with a rich acidic amino acid KDEL sequence that functions in ER retention based on a signal peptide sequence at the N-terminal for guiding the polypeptide into the ER lumen [13][15].

Many PDI family members, such as ERP57, PDIp, P5, ERP72, PDIR, and PDI-D proteins, have been well studied in higher eukaryotes, especially in mammals. These proteins not only act as redox catalysts and isomerases, but also share other functions including peptide binding, cell adhesion, and chaperone activities [16]. Phylogenetic analyses of these sequences with thioredoxin (TRX) domains in higher plants placed the PDIL multi-gene family members into at least eight subfamilies that can be merged into three major categories on the basis of different compositions of proteins with thioredoxin (TRX) domains [9], [17]. The I, II, III, and VII subfamilies in particular were included in clade I, and in addition to group VII, all had two thioredoxin active domains. Clade II, including subfamilies IV and V with VI and VIII as outliers, demonstrated a high degree of differentiation [17].

PDIs are ubiquitously expressed in almost all tissues and catalyze the formation of intra- and inter-chain disulfide bonds [18], [19]. They play important roles in the maturation of secreted plasma membrane and storage proteins [9]. Twelve, 12, and 21 different PDI genes have been annotated in Oryza sativa, Zea mays, and Glycine max, respectively [17]. Investigations of rice mutant esp2 suggested that OsPDIL1-1 retains proglutelin to prevent heterotypic interactions with prolamine polypeptides within the ER lumen [20], perhaps an important step in starch synthesis [21]. Over-expression of PDIs and BiPs in developing maize endosperm leads to structural changes in storage proteins; therefore, it is possible that PDIs play important roles in the synthesis and association of protein bodies, or in the interaction of β- and γ-zeins with α-zeins [22]. Different expression levels of PDI family proteins in developing cotyledons of soybeans indicate that they may play specific roles at different stages [23], [24]. GmPDIL-1 and GmPDIL-2 serve as molecular chaperones in supporting the correct folding of glycinin or β-conglycinin in the ER of cotyledon cells [24]. Peak expression of GmPDIL-3a and GmPDIL-3b during seed maturation indicates that they might be involved in folding or accumulation of storage proteins [25]. AtPDIL2-1 in Arabidopsis affects ovule structure and promotes embryo sac development through correct guidance of pollen tube growth [26]. In addition, AtPDI5 (AtPDIL1-1) chaperones and inhibits Cys proteases during programmed cell death (PCD) of the endothelium in developing seeds [27]. A new function of PDI in Arabidopsis was found in biogenesis of transitory starch [28]. The PDI and PDIL proteins also play important roles in the chloroplast, and achloroplast-localized disulfide isomerase (cPDI) provides redox potential to regulate activator proteins binding to the 5′UTR of psbA mRNA in chloroplast transcripts [29]. In wheat, nine PDI and PDIL genes were cloned, and their transcriptional levels in endosperm cellularization demonstrated that they were associated with storage protein synthesis and deposition, which is highly related to wheat gluten quality [17].

Abiotic stresses, such as response to chemical reagents, hormones, drought, and high salinity significantly affect plant growth and development. Some PDI family members are induced to improve protein folding and transport during stress. In Arabidopsis, 6 genes (AtPDI1-1, AtPDI1-2, AtPDI2-1, AtPDI4-1, AtPDI5-1, and AtPDI5-2) were up-regulated in response to well-documented chemical inducers of UPR, viz.: DTT, Tm, and Me [30]. Maize PDI genes are also more highly expressed under dehydration, cold, salt, and abscisic acid (ABA) stresses [31]. In wheat, TaPDI1, TaPDI2, and TaPDI3 showed highly up-regulated expression under drought, heat, and cold stresses in roots and other tissues [32].

As a member of the Pooideae subfamily and a temperate wild annual grass endemic to the Mediterranean and Middle East, B. distachyon has rapidly become a new model plant for temperate grass species such as wheat and barley, and in recent years it has been studied extensively. Although PDI proteins play crucial roles in plant growth and development, little has been reported about this family in B. distachyon. Here we report the first molecular characterization, phylogenetic evolution, and expression profiles of PDI genes in B. distachyon in different tissues and under various stresses. Our results provide new insights into the molecular structures, phylogenetic evolution, and functions of the PDI gene family in B. distachyon.

Results

In silico identification of PDI and PDIL genes in B. distachyon

A total of 11 B. distachyon PDI genes were confirmed and assigned to 5 different Brachypodium chromosomes on the basis of the database search results (Figure 1A). Each chromosome had at least two PDI genes regardless of size. Plant Genome Duplication Database (PGDD) analysis confirmed that the BdPDIL4-1 and BdPDIL4-2, and BdPDIL7-1 and BdPDIL7-2 pairs were duplicated sequences. BdPDIL4-1 and BdPDIL4-2 were located on the same chromosome but were physically well separated, whereas BdPDIL7-1 and BdPDIL7-2 were located on different chromosomes. These genes might have originated from duplication of chromosomal segments. BdPDIL1-2 was tightly linked with BdPDIL7-2 on chromosome 5, but both shared higher similarity in amino acid sequences with BdPDIL1-1 than with each other. Later phylogenetic analysis placed BdPDIL1-2 and BdPDIL1-1 in the same subfamily. Interestingly, BdPDIL1-2 had no duplicated sequences, suggesting that these genes originated from different progenitors. Exon/intron analysis also showed that three pairs of BdPDIL genes (BdPDIL1-1 and BdPDIL1-2; BdPDIL4-1 and BdPDIL4-2; and BdPDIL7-1 and BdPDIL7-2) shared similar exon/intron structures (Figure 1B).

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Figure 1. Chromosome distribution and exon-intron structures of 11 B. distachyon PDI and PDI-like genes.

(A) Chromosome numbers are indicated at the top of each bar; the scales show their size (Mb). Red and purple triangles indicate the upward and downward direction of transcription, respectively. Blue dotted lines connect the PDI genes present duplicate chromosomal segments. (B) Green boxes represent exons. The black solid lines connecting two exons represent introns, and the blue boxes represent upstream/downstream sequences. The grid scales show the gene sizes (kb).

https://doi.org/10.1371/journal.pone.0094704.g001

The corresponding locus and genetic characteristics of BdPDI and BdPDIL genes are shown in Table 1. BdPDIL1-1 had 518 amino acids and molecular mass of 56.79 kDa; BdPDIL3-1 (543 aa) was the largest PDIL protein, whereas BdPDIL6-1 (151 aa) was the smallest.

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Table 1. Characteristics of 11 Brachypodium distachyon PDI and PDI-like proteins.

https://doi.org/10.1371/journal.pone.0094704.t001

Phylogenetic analysis

To investigate the phylogenic relationships of PDI and PDIL genes between B. distachyon and 10 other plant species and to generate an evolutionary framework, an unrooted phylogenetic tree was constructed from alignment of 137 PDI and PDIL amino acid sequences (File S1), including 11 from B. distachyon (Bd), 9 from Triticum aestivum (Ta), 7 from Hordeum vulgare (Hv), 7 from Aegilops tauschii (Ae), 12 from Oryza sativa (Os), 12 from Zea mays (Zm), 21 from Glycine max (Gm), 13 from Arabidopsis thaliana (At), 11 from Sorghum bicolor (Sb), 22 from Brassica campestris (Bc), and 12 from Populus trichocarpa (Pt). As shown in Figure 2, three major clades and eight phylogenetic groups (I–VIII) were clearly separated among the plant PDI family. The largest, clade 1, included subfamilies I, II, III, and VII and 71 PDI and PDIL genes, whose members contained two active TRX domains at the N- and C-terminal ends. Subfamily I included the typical PDI, which had been published in several plant species. In addition, the VII subfamily proteins possessed only an N-terminal active domain. Evolutionary relationships indicated that these subfamily members may originate from a common progenitor gene, in which the VII subfamily would have emerged by loss of the C-terminal active domain. Clade 2 contained subfamilies IV and V, consisting of 34 PDI and PDIL genes whose proteins possessed two tandem thioredoxin active domains at the N-terminal end. As outgroups, subfamilies VI and VIII with 32 PDI and PDIL genes were included in clade 3; these had a single active thioredoxin domain, suggesting that they underwent greater divergence during evolution.

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Figure 2. Phylogenetic tree showing relationships between the deduced amino acid sequences of 137 PDI and PDI-like genes from different plant species.

11 from Brachypodium distachyon (Bd), 9 from Triticum aestivum (Ta), 7 from Hordeum vulgare (Hv), 7 from Aegilops tauschii (Ae), 12 from Oryza sativa (Os), 12 from Zea mays (Zm), 21 from Glycine max (Gm), 13 from Arabidopsis thaliana (At), 11 from Sorghum bicolor (Sb), 22 from Brassica campestris (Bc),and 12 from Populus trichocarpa (Pt). Multiple alignments of sequences were performed by ClusalW, and the phylogenetic tree was constructed by the neighbour-joining (NJ) method and evaluated by bootstrap analysis. Numbers on the main branches indicate bootstrap percentages for 1,000 replicates. The three major clades (1–3) and eight phylogenetic groups (I–VIII) identified in the plant PDI family are highlighted with a red arc and the same color branch, respectively.

https://doi.org/10.1371/journal.pone.0094704.g002

BdPDI and BdPDIL protein structure and motif analysis

Structural characteristics of the 11 BdPDI and BdPDIL proteins (Table 2) were searched using different protein databases; the multiple sequence alignments of thioredoxin-like domains are shown in Figure 3. The conserved motifs of PDI family members were investigated using Meme v4.9 as shown in Figure 4. All BdPDI and BdPDIL proteins had at least a thioredoxin-like domain with the -CXXC- catalytic site necessary for isomerase and redox activities. Motifs 1 and 3 are a fundamental structural combination in all BdPDI family members. In Arabidopsis and rice, the homologous domains (motifs1-3) involved in catalyzing protein disulfide bond formation and isomerization are contained in the homologous PDI and PDIL proteins, and their locations are similar to B. distachyon (Figure A and B in File S2). In addition, a high-affinity substrate-binding site in the b′ domain modulating the pKa of the two conserved cysteine active sites and a glutamic acid-lysine charged pair involved in proton transfer reactions are prominent determinants of the enzymatic activity of PDI family members [33].

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Figure 3. Motif analysis was performed using MEME 4.90 software as described in the methods.

(a) Three kinds of motifs were included in the a and a′ domains, which were homologous to thioredoxin (TRX) domains. Motifs 1 and 2 contained single CxxC catalytic motifs. (b) Motif 3 was closely linked with motifs 1 and 2 and contained cis pralines (P) near each active site that might be crucial for the catalytic activity of thioredoxin or other functions.

https://doi.org/10.1371/journal.pone.0094704.g003

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Figure 4. Multiple sequence alignment of a-type domains of B. distachyon PDI and PDI-like proteins and a typical rice PDI.

These thioredoxin-like domains of the B. distachyon were annotated in Phytozome database, and comparative analysis used BioEdit software. Residues highlighted in deep blue and green show they were identical and similar, respectively. Open bars and arrowheads represent the α helices and β strands, respectively. The red box indicates the -CxxC- catalytic site, and red arrows indicate the glutamicacid–lysine charged pair. Blue and yellow arrows represent the conserved arginine (R) and the cis pralines (P) near the active site, respectively.

https://doi.org/10.1371/journal.pone.0094704.g004

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Table 2. Structural and functional characteristics of 11 B. distachyon PDI and PDI-like proteins.

https://doi.org/10.1371/journal.pone.0094704.t002

To better understand structural characteristics, the tertiary structure of a typical B. distachyon PDI protein BdPDIL1-1 was predicted by the Phyre2 server and some important amino acids were indicated (Figure 5). The overall structure of BdPDIL1-1 consisted of five domains and one linker (abb′xa′c) in the shape of a twisted “U”, similar to the structure of yeast PDI, in which two pairs of active sites facing each other across the long sides and the inside surface of the “U” are enriched in hydrophobic residues that would benefit interaction with unfolded or misfolded proteins [34], [35].

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Figure 5. Overall structure of B. distachyon PDIL1-1 protein.

The tertiary structure was predicted by the Phyre2 server, and the abb′xa′c (five domains and one linker) structure composition indicated similarity with the structure of human and yeast PDI. The -CXXC- catalytic sites are indicated by green and red spheres. The secondary structure is shown with α helixes in red, β sheets in yellow, and loops in green. Some important amino acid (glutamicacid–lysine charged pair and conserved arginine) are marked near each active site on the basis of the characteristics of human PDI.

https://doi.org/10.1371/journal.pone.0094704.g005

Two homologous genes (BdPDIL1-1and BdPDIL1-2) were included in subfamily I. They encode typical PDI proteins with a multi-domain, including the a-b-b′-a′ thioredoxin-like domain, the 26 aa N-terminal signal peptide, and the C-terminal KDEL signal that guides polypeptide translocation and retention in the ER. In addition, both PDI proteins also contain the -CGHC- motif of the active site (motifs 1 and 2), two charged glutamic acid-lysine pairs (E65-K99 and E409-K442 in BdPDIL1-1; E59-K93 and E403-K436 in BdPDIL1-2), and the conserved arginine residues (R139 and R478 in BdPDIL1-1, R133 and R473 in BdPDIL1-2) involved in modulating the pKa of the cysteine residue active-site as shown in Figure 4.

Subfamilies II and III had only family members BdPDIL2-1 and BdPDIL3-1, respectively. In addition to similar multi-domains, an acidic amino acid–rich sequence named c was present in the N-terminus in both subfamilies. In Chlamydomonas reinhardtii, the PDI-like protein (RB60) depended on the N-terminal acidic domain in the chloroplast, which regulated light-induced translation of chloroplast mRNAs through its redox activity [36], [37]. However, BdPDIL3-1 showed some different characteristics: the thioredoxin-box-CGHC- motif was replaced by -CERS- and -CVDC- motifs. Besides, the glutamic acid in the a domain was changed into a leucine residue and arginine was replaced by histidine, whereas the charged lysine in the a′ thioredoxin domain became arginine and the conserved arginine residues were replaced by leucine. These amino acid changes may result in changes in biochemical properties and functions.

The members of subfamilies IV and V contained BdPDIL4-1, BdPDIL4-2, and BdPDIL5-1, and both had N-terminal signal sequences and two tandem thioredoxin domains (-a). In the a thioredoxin domain of BdPDIL4-1 and BdPDIL4-2, one of the lysines in two charged glutamic acid-lysine pairs was replaced by L-asparagine, and two conserved arginine residues were present (R125 and R244 in BdPDIL4-1; R127 and R246 in BdPDIL4-2). In addition, an about 100 aa D domain was close to the C-terminus, and the C-terminal retrieval sequence -H/KDEL became -TFSS and -IFSS in BdPDIL4-1 and BdPDIL4-2, respectively. In the D domain of D. discoideum PDI proteins, the 57-residue sequence is necessary and sufficient for ER localization, implying that the D domain might play a ubiquitous role in retrieval or retention of ER residues to make up for the lack of an H/KDEL-type retrieval sequence [38]. BdPDIL5-1 had two conserved arginine residues (R119 and R257), an inactive thioredoxin b domain at the C-terminus, and an -NDEL retrieval sequence for its ER localization; however, glutamic acid-lysine charged pairs near the -CGHC- active site in the -a thioredoxin domain was replaced by alanine and histidine, respectively.

In subfamily VII, two homologous PDI members with similar structural features, BdPDIL7-1 and BdPDIL7-2, were included in clade 1, but they retained only single thioredoxin domains and lacked the H/KDEL-type retrieval sequence. The glutamic acid-lysine charged pair was replaced by D-aspartic acid (D63-K97 and D69-K103), and the conserved arginine (R133 and R139) was retained near the -CGHC- active site. Although they lack the H/KDEL-type retrieval sequence, the PDI proteins could be retained in the ER depending on the C-terminal transmembrane segment.

BdPDIL6-1 and BdPDIL8-1 were classified into clade 3 as the outlying subfamily. As the smallest subfamily member in B. distachyon, BdPDIL6-1 had a peptide sequence and transmembrane segment in the N-terminus, a single thioredoxin domain, and a -QDEL retrieval sequence for retention in the ER. In addition, the charged glutamic acids were replaced by glutamine. BdPDIL8-1 showed a different structure than other subfamily members, including a non-characteristic tetra-peptide active site -CYWS sequence and two trans-membrane region sequences. An endoplasmic reticulum-Golgi intermediate compartment (ERGIC) domain was located in the N-terminus, and an endoplasmic reticulum vesicle transporter domain (COPII coated_ERV) was located in the C-terminus. These domains are also present in several other proteins, such as ERGIC-32 in mouse and Erv41p and Erv46p in yeast, and play important roles in protein sorting, folding, and glycoprotein processing in the ER and early Golgi complex [39], [40]. The functions of two trans-membrane regions of the BdPDIL8-1 are assumed to replace the function of the N-terminal signal peptide and C-terminal KDEL retrieval sequence, both of which are involved in the early protein secretory pathway between ER, ERGIC, and the Golgi complex.

According to the type of glycosyl chain, two possible types of glycosylation were predicted: O-linked glycosylation and N-linked glycosylation. In yeast and several mammalian species, the PDI might serve as glycoproteins. More credible evidence confirmed that wheat PDIL1-1 is a glycoprotein that retains a glycosylation site in the amino acid sequence [41], [42], suggesting that some BdPDI proteins with putative O/N-glycosylation sites also could be glycosylated.

BdPDI and BdPDIL gene promoter analysis

Regulation of PDI and PDIL gene transcription levels in diverse metabolic activities depends on interaction of their cis-acting regulatory elements in upstream promoter sequences with different transcription factors [43]. The 2000 bp promoter sequences upstream of the initiation codon of the 11 BdPDI and BdPDIL genes were searched for cis-acting regulatory elements by the Plant CARE database (File S3). These cis-acting regulatory elements are mainly related to three important physiological processes: the light cycle, hormonal/environment responses, and seed-specific gene expression. A large number of light-responsive elements were present in the promoter region, suggesting that the PDI and PDIL genes play important roles in photosynthesis or carbohydrate metabolism. Some other important cis-acting regulatory elements are shown in Table 3. Three important seed-specific expression cis-motifs (Skn-1_motif, GCN4_motif, and RY-element) were conserved in the promoter regions of some BdPDI and BdPDIL genes; these are involved in regulating gene expression of cereal grain storage proteins [44], [45]. Transcription levels of PDI genes with these regulatory motifs were higher in immature caryopses than in other tissues. Some stress-related cis-acting elements, such as ABRE, MBS, TC-rich repeats, G-Box, and 5′UTRPy-rich stretch, were also present in the PDI promoter region. In Oryza sativa, the frequent presence of five cis-motifs in the promoter region of oxidative defense pathway genes suggests that PDI genes with these motifs are involved in stress defense [46]. All cis-acting regulatory elements could individually or interactively regulate expression of BdPDI and BdPDIL genes in plant growth and development or against various environmental stresses.

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Table 3. Functional motif numbers of cis-regulatory elements identified in PDI and PDI-like genes of B. distachyon.

https://doi.org/10.1371/journal.pone.0094704.t003

Differential expression of PDI and PDIL genes in different organs of B. distachyon

PDIs are types of ubiquitously expressed proteins that occur in a variety of tissues [47]. To understand the organ-specificity of PDI family members in B. distachyon, expression levels of the 11 BdPDI and BdPDIL genes in different organs, including roots, stems, and leaves at the two-leaf and heading stages; paleas; lemmas; seeds; and developing caryopses were investigated by qRT-PCR (Figure a, b, c in File S4). The normal expression level of BdPDIL1-2 was too low to be detected effectively, but it showed higher expression levels under salt and drought treatments.

As shown in Figure 6 and Figure a, b, c in File S4, all BdPDI and BdPDIL genes were detected in six different tissues, but with significantly different expression levels at different developmental stages and tissues. BdPDIL2-1, BdPDIL3-1, and BdPDIL7-2 showed higher expression levels in roots, stems, paleas, and lemmas at the heading stage, whereas BdPDIL4-2 was abundant in roots, stems at the two-leaf stage, and early stages of seed development. BdPDIL1-1and BdPDIL5-1 showed higher expression levels in caryopses compared with other organs. BdPDIL6-1 and BdPDIL8-1 displayed continuously high expression patterns in caryopses, whereas BdPDIL4-1 and BdPDIL7-1 exhibited similar expression profiles in all tissues.

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Figure 6. Expression profiling of PDI and PDIL genes in different Brachypodium distachyon organs.

(a) Comparative expression levels of 10 PDI and PDI-like genes in different Brachypodium distachyon organs, including roots (R1), stems (S1), and flag leaves (FL1) at the two-leaf stage, stem (S2) and flag leaf (FL2) at heading with 1 cm section of panicle from the leaf sheath; seed palea at 11 and 23 days after anthesis (P11A and P23A); seed lemma at 11 days after anthesis (L11A), and caryopses at 10 days post-anthesis (10 DPA). (b) Dynamic expression profiles of 10 PDI and PDI-like genes during seed development in Bd21. Relative quantification of the expression levels in developing caryopses was collected between 4 and 30 DPA. Expression data were obtained from three biological replicates. The relative expression levels at 10 DAP were set to value 1 as the calibrator in the pictures a and b.

https://doi.org/10.1371/journal.pone.0094704.g006

Dynamic transcriptional expression levels of 10 BdPDI and BdPDIL genes from the B. distachyon PDI family at 12 different grain developmental stages were investigated by qRT-PCR, and their expression profiles are shown as heatmaps in Figure 6b. The sampled caryopses covered stages of endosperm development from cellularisation to desiccation. Ten BdPDI and BdPDIL genes displayed three main expression patterns. The first involved five PDIL genes (PDIL1-1, PDIL2-1, PDIL5-1, PDIL6-1, and PDIL8-1) and generally showed up-to-down expression trends, although slight expression differences were present; for example, expression of typical PDI gene PDIL1-1 increased gradually from 4 DPA to its highest value at 8 DPA, then gradually decreased until 16 DPA, after which its expression level increased dramatically again and reached its second highest peak at 18 DPA. Along with seed dehydration, its expression level gradually decreased and reached its lowest level at 30 DPA. Three BdPDIL genes (BdPDIL3-1, BdPDIL4-2, and BdPDIL7-2) displayed a different expression pattern with much higher expression levels during early grain development stages (4–6 DPA), then decreased slightly or remained at relatively low levels until 14 DPA. In the following grain development stages, the genes exhibited up-down expression patterns from 16 to 30 DPA, with the highest level at 20 DPA. The remaining BdPDIL4-1 and BdPDIL7-1 showed a third expression pattern: gradual up-regulation with the highest level at 30 DPA.

Expression profiles of PDI and PDIL genes under abiotic stresses

Under natural conditions, a variety of adverse environments, such as drought, salinity, high temperature, and chilling, affect plant growth and development. Artificial stress environments help explore how plants adapt to environmental stress by adjusting morphological, physiological, and molecular mechanisms. The transcriptional expression profiles were obtained for the 11 BdPDI and BdPDL genes in seedling leaves subjected to various abiotic stress environments, including treatment with 200 mM PEG6000, 160 mM salinity, 0.1 mM ABA, and 20 mM H2O2.

Under drought stress induced by PEG 6000, 4 genes (BdPDIL1-1, BdPDIL1-2, BdPDIL7-2, and BdPDIL2-1) were significantly up-regulated, whereas 3 genes (BdPDIL3-1, BdPDIL5-1 and BdPDIL8-1) were significantly down-regulated (Figure 7a and Figure a in File S5). All BdPDI and BdPDIL genes were significantly up-regulated at 12 h under salinity treatment. Expression of 6 genes (BdPDIL3-1, BdPDIL4-1, BdPDIL4-2, BdPDIL5-1, BdPDIL6-1, and BdPDIL8-1) began to down-regulate at 24 h under salinity treatment (Figure 7b and Figure b in File S5). Only BdPDIL1-1 expression was significantly up-regulated at 2 h under H2O2 treatment; the others were significantly down-regulated until 6 h (Figure 7c and Figure c in File S5). Under ABA treatment, the expression of BdPDIL1-1 was significantly up-regulated, whereas 6 genes (BdPDIL2-1, BdPDIL3-1, BdPDIL4-1, BdPDIL4-2, BdPDIL6-1, and BdPDIL7-2) showed significantly down-regulated expression (Figure 7d and Figure d in File S5). Interestingly, the typical PDI gene BdPDIL1-1 was significantly up-regulated under all four stress treatments (Figure 7 a–d and Figure a-d in File S5).

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Figure 7. Expression profiles of BdPDI family members in the leaves of B. distachyon in response to drought, salt, H2O2 and ABA, treatments using real-time quantitative RT-PCR and Cluster 3.0 and Java Tree View programs.

Blocks with colors indicated decreased (green) or increased (red) transcript accumulation relative to the respective control. The gene expression patterns were labeled in red (up-regulated), green (down-regulated), and blue (up- or down-regulated in different times). Filled squares indicated a significant difference from the control (P<0.05) using SPSS (Statistical Product and Service Solutions) software. Expression profiles of the BdPDI and PDIL genes under: a. drought stress for 12 h and 24 h; b. salinity stress for 12 h and 24 h; c. H2O2 stress for 0, 2, 4 and 6 h; d. ABA stress for 6 h.

https://doi.org/10.1371/journal.pone.0094704.g007

Discussion

Molecular characterization and phylogenetic relationships of the PDI and PDIL family of B. distachyon compared with each other and with other plant species

Eleven PDI and PDIL genes were evenly distributed across the five chromosomes of Brachypodium; the pairs BdPDIL4-1 and BdPDIL4-2 as well as BdPDIL7-1 and BdPDIL7-2 shared similar exon/intron structure and motif organizations (Figures 1 and 4). PGDD analysis also confirmed that the two pairs were segmentally duplicated sequence pairs that likely originated from the same progenitor genes; thus, the 11 BdPDI and BdPDIL genes likely evolved from at least 8 progenitor genes. Protein structure and motif analyses displayed the structure and sequence changes of subfamily members I-VIII. Open reading frames of different size and partial motif deletions and mutations of some important amino acids showed that they had likely undergone a complex evolutionary process involving unequal recombination, duplication, and deletion of gene fragments. These changes influenced their respective functions significantly.

Estimates of divergence times of Brachypodium and cultivated crops are 32–39 million years ago (MYA) for wheat, 40–53 MYA for rice, and 45–60 MYA for sorghum [48]; hence, the genetic relationship of B. distachyon is much closer to wheat than to rice and sorghum. The phylogenetic tree also showed that BdPDIL1-1, BdPDIL4-2, BdPDIL5-1, BdPDIL6-1, and BdPDIL7-1 genes are much closer to those of wheat than rice or sorghum (Figure 2). PDI and PDIL members from monocots (wheat, rice and maize, barley, sorghum, B. distachyon, and Ae. tauschii) and dicots (Arabidopsis, soybean, poplar, and Brassica campestris) generally form two distinct subgroups (Figure 2). Two dicot genes (PtPDIL4-1 and PtPDIL4-2) from Populus trichocarpa in subfamily IV, however, were very close to 5 monocots (ZmPDIL5-1, OsPDIL5-1, GmPDIL5-1, GmPDIL5-2, and SbPDIL5-1) in subfamily V from maize, rice, soybean, and sorghum. This result indicates that a few plant PDI genes in subfamilies IV and V are highly conserved in both monocots and dicots; thus, we hypothesize a common evolutionary origin for the plant PDI family in which the PDI genes from monocots and dicots diverged from a single ancestral gene long before divergence through a series of genome segmental duplications and deletions, chromosome fusions and translocations, and ultimately generation of multi-gene PDI families.

Organ-specificity and dynamic expression profiling of PDI and PDIL genes during grain development and their effects on storage protein synthesis

Transcript expression analysis of PDI family members in six different tissues as revealed by qRT-PCR confirmed that their expression was not organ-specific, which is consistent with most reports [18], [19]. The PDIs play different roles in the maturation of secreted plasma membrane and storage proteins [9]; however, the expression levels of individual PDI family members display greater differentiation. Some members, such as BdPDIL1-1and BdPDIL5-1, showed higher expression in grains, whereas others, such as BdPDIL3-1, showed higher expression levels in other organs (Figure 6), implying that they have specific roles in different organs or different stages of plant development.

The dynamic expression patterns of BdPDI and BdPDIL genes during seed development are useful for further understanding the molecular mechanisms of the PDI family in protein folding networks, synthesis, and deposition of polymers. As in other cereal crops, grain development from flowering to harvest in B. distachyon goes through three stages: embryogenesis, maturation, and dehydration. In this process, PDI and PDI-like proteins play important roles in the correct assembly of both intra-chain and inter-chain disulphide bonds, protein folding, and assembling and accumulating protein bodies. Initial studies in B. distachyon showed very low amounts of prolamins in the grains and the main storage proteins were 11S and 7S globulins [49], [50]. Recent studies have found that Brachypodium seeds nevertheless contain LMW-GS as well as much lower amounts of HMW-GS [51], [52].

During embryo genesis, seed metabolism is very active as are many metabolic enzymes, such as β-amylase, xyloglucan endotransgly cosidase, and hydrolase [53]. At an early embryogenesis stage (4–6 DPA), four BdPDIL genes (BdPDIL3-1, BdPDIL4-2, BdPDIL7-2, and BdPDIL8-1) showed high expression levels, with maxima occurring earlier than some amylase genes (Figure 6b), implying that they could be involved in folding and assemby of these functional proteins in preparation for starch synthesis or other metabolic activities. At about 13 DPA, accumulation of storage protein, such as 11S globulin [53], was detected. Expression levels of BdPDIL1-1, BdPDIL2-1, BdPDIL4-1, and BdPDIL5-1 increased rapidly and reached the first maximum at 8 and 10 DPA, before synthesis of storage proteins, indicating that these PDI proteins play important roles in assisting the formation of intra-chain disulfide bonds in storage proteins. The second peaks of transcription expression occurred at about 20 DPA, when protein synthesis and accumulation increased dramatically and when much larger protein vesicles were distributed in the cytoplasm, suggesting that they were involved in the mass formation of intra-chain and inter-chain disulfide bonds. Promoter analyses also showed that some cis-acting regulatory elements required for endosperm expression were present in these genes (Table 3); moreover, four orthologous soybean and wheat PDI genes had similar functions in the folding of seed storage proteins [54], [55].

BdPDIL4-1 and BdPDIL7-1 displayed their highest expression levels at the late stage of grain development (about 30 DPA), coinciding with the beginning of seed desiccation and coalescence of large protein vesicles, suggesting that these PDI proteins may be involved in formation or rearrangement of inter-chain disulfide bonds. TaPDIL7-1 in wheat shared a similar expression pattern and was shown to play an important role in disulphide bond formation at later stages of grain development [55]. Even though BdPDIL4-1 and BdPDIL4-2 as well as BdPDIL7-1 and BdPDIL7-2 were paired duplication sequences with high similarities in amino acid and exon/intron structural organization, their different expression patterns within pairs indicate that functional differentiation occurred during the evolutionary process.

Expression features and potential functions of PDI and PDIL genes under different abiotic stresses

Synthesis, folding, and sorting of proteins in the ER are dependent on a series of regulatory gene networks. Adverse environments easily disturb the complex physiological processes leading to unfolding or misfolding of ER proteins [56]. In Arabidopsis, 6 genes were up-regulated when induced by dithiothreitol (DTT), beta-mercaptoethanol (β-Me), and tunicamycin (Tm) [30]. Likewise, BiP, SIL1 homolog, peptidyl-prolyl-cis-trans isomerases (cyclophilin), and GRP94 were induced by ER stress in Arabidopsis [57]. These folding-related proteins could play different roles in ensuring the correct folding and assembly of nascent polypeptide chains in the ER (Figure 8).

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Figure 8. Schematic indicating that the PDI proteins might be involved in three major metabolic pathways (UPR, PCD, and protein folding) in the ER under various adverse stresses.

Unfolded proteins response (UPR) and programmed cell death (PCD) induced by the various stresses (cited from reference 56). The PDI proteins catalyzed the formation and rearrangement of disulfide bonds of unfolded or misfolded proteins, but some misfolded proteins still need to be degraded. In Arabidopsis, PDIL1-1 protein as the chaperone inhibits Cys proteases from entering the protein storage vacuoles (cited from reference 27). Dashed arrows indicate incompletely understood relationships that need to be further verified. Upward-pointing blue arrows represent metabolic regulation proteins up-regulated under drought and salt stresses to enhance plant tolerance (cited from references 64–66). CNX/CRT, calnexin/calreticulin proteins; PSV, protein storage vacuoles.

https://doi.org/10.1371/journal.pone.0094704.g008

Up-regulated PDI genes such as BdPDIL1-1 and BdPDIL2-1 in B. distachyon under drought and salt stress contain two active sites, and a C-terminal ER-retention signal could be involved in enhancing protein-folding capacity in the ER. Different BdPDI and BdPDIL genes that displayed apparently different expression patterns under four different stress treatments imply that their functional differentiation might have occurred during a long-term evolutionary process.

Environmental stresses such as salt, drought, abscisic acid, and H2O2 also lead to the accumulation of reactive oxygen species (ROS) in plant cells [58][60]. PDI has an important function in the thioredoxin-based redox pathway and forms part of the antioxidative defense system [61]. Promoter analysis showed that five cis-motifs that occur at high frequencies in the promoter regions of oxidative defense pathway genes are also present in the BdPDIL1-1, BdPDIL2-1, and BdPDIL3-1 gene promoters. Up-regulated expression of these PDI and PDIL genes could be involved in stress defense mechanisms. The different numbers of five cis-motifs in the promoter and structure characteristics may lead to the different expression levels of BdPDIL1-1, BdPDIL2-1, and BdPDIL3-1 under environmental stresses.

Up-regulated expression of BdPDIL1-1 under H2O2 treatment suggests that it could be involved in antioxidative defense. A signal pathway that results in programmed cell death (PCD) is initiated and propagated via increasing accumulation of ROS [62], [63]. ROS-induced PCD is regulated by cysteine proteases. In Arabidopsis, AtPDIL1-1 protein interacts with three different Cys proteases in vitro, suggesting that AtPDIL1-1 as the chaperone inhibits Cys proteases from leaving the ER through the Golgi to vacuoles before the proteases are activated [27], thus delaying the protease entry into the protein storage vacuoles (PSVs), where it degrades the storage proteins (Figure 8).

In wheat, many proteins involved in different metabolic regulation events respond to drought stress, including photosynthesis and the Calvin cycle, cell redox homeostasis, glycolysis and gluconeogenesis, transport and protein-folding mechanisms, protein degradation, and amino acid metabolism [64]. In B. distachyon, some proteins were also involved in drought and salt stress responsive mechanisms, such as cystathionine gamma-synthase, methylthioribose kinase, and asparagines synthase, all of which were strongly up-regulated under drought stress (Figure 7a). Casein kinase I (CKI)-like protein, aminophospholipid ATPase, calcium-transporting ATPase, protein phosphatase 2C, potassium transporter, and calcium-binding protein were also up-regulated in response to salt stress [65], [66]. The PDI proteins are necessary to assist folding of nascent polypeptides to form specific functional proteins that regulate metabolic activities and subsequently result in an increase in plant resistance (Figure 8).

BdPDIL1-1 in B. distachyon is homologous to AtPDIL1-1, ZmPDIL1-1, OsPDIL1-1, and TaPDIL1-1, which are induced by various stress conditions [21], [30][32]. These results provide an important foundation for further functional studies on BdPDIL1-1; however, under direct H2O2 stress treatment, more PDI genes showed down-regulated expression patterns. Low PDI protein expression levels under H2O2 stress indicated that more reduced enzymes (e.g., reduced glutathione) could effectively be involved in rapid detoxification of O2- and H2O2, leading to reduced hydrogen peroxide damage [58]. Even though these stresses have similar negative impacts on plant growth, the BdPDI and BdPDIL genes might play different roles in different pathways or in cooperating with other genes to form networks that resist adverse environmental impacts.

Conclusions

In this study, we identified 11 PDI and PDIL genes in the B. distachyon genome by in silico analysis. Phylogenetic analysis classified them into three clades and eight subfamilies. Different exon/intron organizations, partial motif deletions, and important amino acid mutations showed that they underwent a high degree of differentiation through unequal homologous recombination, gene duplication, and deletion of gene fragments. The different expression patterns of the BdPDI and BdPDIL genes in developing caryopses and under various stress conditions further confirmed that their functions were differentiated due to the changed structures. These observations provide a better understanding of the structures and functions of BdPDI and BdPDIL genes.

Material and Methods

Database searches for identifying PDI family members in B. distachyon and other plant species

To obtain the B. distachyon PDI and PDIL genes, previously cloned sequences of PDI and PDIL genes from rice (12 sequences) and Arabidopsis (13 sequences) were used for a BLAST search of two public databases: Species in Phytozomev9.0 (http://www.phytozome.org/) and NCBI (http://www.ncbi.nlm.nih.gov/). In addition, 11 orthologous PDI genes from Sorghum bicolor, 22 from Brassica campestris, and some of Hordeum vulgare and Aegilops tauschii PDI genes were also collected from the two public databases. Other plant species PDI genes, such as soybean (Glycine max), poplar (Populus trichocarpa), and wheat (Triticum aestivum) were from published results [17].

Chromosomal locations, gene duplication, exon/intron organization analyses of PDI genes, and characteristics of PDI proteins in B. distachyon

The putative PDI protein sequences were further confirmed and analyzed using the PFAM HMMs [67], CDD (http://www.ncbi.nlm.nih.gov/Structure/cdd/cdd.shtml) from NCBI, InterPro (http://www.ebi.ac.uk/interpro/), and ExPASy (http://www.expasy.org/) databases. The gene locations were based on the Phytozome v9.1 datebase and mapped by Map Inspect software. Identification and cataloging of B. distachyon PDI genes in terms of intra-genome or cross-genome syntenic relationships were conducted using the Plant Genome Duplication Database (PGDD) (http://chibba.agtec.uga.edu/duplication/index/locus). Gene transcription directions were searched from Gramene (http://www.gramene.org/Brachypodium_distachyon/Info/Index). The exon/intron organization was analyzed by Gene Structure Display Server (GSDS) (http://gsds.cbi.pku.edu.cn/). The protein pI/Mw were obtained with the Compute pI/Mw tool (http://web.expasy.org/compute_pi/), the presence of signal peptides was confirmed by Signal P4.1 (http://www.cbs.dtu.dk/services/SignalP/), and transmembrane regions were determined by TMHMM ver 2.0 (http://cbs.dtu.dk/services/TMHMM-2.0/) and SMART databases (http://smart.emblheidelberg.de/). N-/O-glycisilation sites and phosphorylation sites were predicted by NetNGlyc 1.0 (http://www.cbs.dtu.dk/services/NetNGlyc/), NetOGlyc 3.1 (http://www.cbs.dtu.dk/services/NetOGlyc/), and NetPhos 2.0 Server (http://www.cbs.dtu.dk/services/NetPhos).

Phylogenetic analysis

A total of 137 PDI and PDIL sequences from 11 plant species were used to construct a phylogenetic tree. The sequences and respective protein ID or transcript names are displayed in File S1 and S2, and the corresponding nomenclatures were composed of two letters for genus and species, followed by PDIL and an Arabic number. The PDI and PDIL amino acid sequences of the whole coding regions were aligned by Clustal W parameters using the Gonnet series as the protein weight matrix and parameters set to a 5-gap open penalty, 0.55-gap extension penalty, 4-gap separation distance, negative matrix, and end-gap separation on and divergent sequences delay at 20%. The phylogenetic tree was constructed using MEGA software 5.10 [http://www.megasoftware.net/] with the neighbour-joining (NJ) method and 1,000 bootstrap replicates with the bootstrap method.

Multiple sequence alignment, tertiary structure prediction, conserved motifs, and promoter analysis of BdPDI and BdPDIL genes

Protein sequence alignment was performed by BioEdit software (http://www.mbio.ncsu.edu/bioedit/bioedit.html). Conserved motifs of PDI family members were investigated using Meme v.4.9 (http://meme.nbcr.net/meme/cgi-bin/meme.cgi). The tertiary structure of B. distachyon PDIL1-1 protein was predicted by Phyre2 Server (http://www.sbg.bio.ic.ac.uk/phyre2/html/page.cgi?id=index). The promoter regions were analyzed according to 11 BdPDI and BdPDIL genes from the B. distachyon database with Phytozomev.9.0. Two thousand bp regions upstream of the PDI genes were used in promoter searches for cis-acting regulatory elements based on the Plant CARE database (File S3) (http://bioinformatics.psb.ugent.be/webtools/plantcare/html/).

Plant growth, stress treatments, and sample harvest

Brachypodium distachyon 21 (Bd21) seeds were sterilized with 75% alcohol and 15% sodium hypochlorite, rinsed 4–5 times, and placed on moistened filter paper in Petridishes and germinated at 26°C for one week. Ten seedlings were transferred to pots in a growth room at 22°C and a 16 h day/8 h night photoperiod. When the seedlings reached the two-leaf stage, drought, high salinity, ABA, and H2O2 treatments were initiated. Drought treatment was conducted with 200 mM polyethylene glycol 6000 for 12 and 24 h; salt treatment was 160 mM sodium chloride treatment for 12 and 24 h; 0.1 mM ABA treatment was for 6 h; and 20 mM H2O2 treatment was for 2, 4, and 6 h. Control and treated leaves were harvested for assays. Developing caryopses were sampled from 4 to 30 days after anthesis (DAA) at 2–5-day intervals (12 sampling times). All samples were immediately frozen in liquid nitrogen and kept at −80°C prior to RNA isolation.

qRT-PCR

Total RNAs were extracted using TRIzol reagent (Invitrogen) according to the manufacturer's instructions. The Prime Script RT Reagent Kit with gDNA Eraser was used for RNA purification and reverse transcription following the manufacturer's instructions. Transcription levels of PDI family genes in three biological replicates for all treatments were quantified by real-time quantitative reverse transcriptional PCR (qRT-PCR) with a CFX96 Real-Time PCR Detection System (Bio-Rad) using SYBR-green as the intercalating dye and the 2(-Delta Delta C(T)) method [68]. Primer pairs for qRT-PCR analysis (Table a in File S6) were designed by the Primer3Plus program (http://www.bioinformatics.nl/cgi-bin/primer3plus/primer3plus.cgi). PDI primer pairs were checked by blasting primer sequences in the NCBI database (http://www.ncbi.nlm.nih.gov/tools/primer-blast/index.cgi?LINK_LOC=BlastHome), and all primers were specifically consistent with the respective sequence of its targeted PDI gene. Real-time melting temperature curves for each BdPDI gene showed single peaks and were confirmed by agarose gel electrophoresis (Figure b in File S6). qRT-PCR efficiency was determined by five serial five-fold dilutions of cDNA, and the standard curve confirmed them at high RT-PCR efficiency rates (Figure a, b, c in File S7). Ubi4 (Bradi3g04730) was used as the reference gene according to previous report [69].

Supporting Information

File S1.

One hundred and thirty-seven PDI and PDI-like amino acid sequences from 11 species used for constructing phylogenetic tree. 11 from Brachypodium distachyon (Bd), 9 from Triticum aestivum (Ta), 7 from Hordeum vulgare (Hv), 7 from Aegilops tauschii (Ae), 12 from Oryza sativa (Os), 12 from Zea mays (Zm), 21 from Glycine max (Gm), 13 from Arabidopsis thaliana (At), 11 from Sorghum bicolor (Sb), 22 from Brassica campestris (Bc), and 12 from Populus trichocarpa (Pt).

https://doi.org/10.1371/journal.pone.0094704.s001

(DOCX)

File S2.

Motif, exon/intron structure organizations, and locations in respective sequences of PDI and PDIL family members in Arabidopsis thaliana (A) and Oryza sativa (B).

https://doi.org/10.1371/journal.pone.0094704.s002

(TIF)

File S3.

Functional motif numbers of identified cis-regulatory elements in PDI and PDIL genes of Brachypodium distachyon.

https://doi.org/10.1371/journal.pone.0094704.s003

(XLSX)

File S4.

Organ-specific expression of Brachypodium PDI and PDIL genes in roots, stems, leaves, paleas, lemmas and developing caryopses. The relative expression levels at 10 DAP were set to value 1 as the calibrator in the pictures a and b.

https://doi.org/10.1371/journal.pone.0094704.s004

(TIF)

File S5.

Relative expression levels of BdPDI family members in the leaves of B. distachyon in response to drought (a), salt (b), H2O2 (c) and ABA (d) stress were analyzed using quantitative RT-PCR and compared with well-watered control plants. The right side of illustrations indicated the treatment time (hour) under corresponding abiotic stresses. Error bars represented the standard deviations of three biological replicates.

https://doi.org/10.1371/journal.pone.0094704.s005

(TIF)

File S6.

Primer sequences used for real-time quantitative RT-PCR (qRT-PCR).

https://doi.org/10.1371/journal.pone.0094704.s006

(DOCX)

File S7.

qRT-PCR optimization design: double standard curve and dissolution curve of BdPDI and BdPDIL genes in different developing organs (a) developing caryopses (b) and leaves under drought, salt, H2O2 and ABA treatments (c). One of the red standard curves represented BdPDI genes and other blue standard curve represented the reference gene. The dissolution curves of different genes were indicated.

https://doi.org/10.1371/journal.pone.0094704.s007

(TIF)

Acknowledgments

We are grateful to Professor Robert McIntosh, University of Sydney, for constructive suggestions in reviewing the manuscript.

Author Contributions

Conceived and designed the experiments: YY YH. Performed the experiments: CZ NL MH GC. Analyzed the data: CZ NL MH GC. Contributed reagents/materials/analysis tools: CZ GC MH. Wrote the paper: CZ JL YY. Helped draft the manuscript: YY YH. Performed the preparation of cDNA, qRT-PCR, and bioinformatics analyses: JZ GY XL. Helped manuscript writing and English editing: JL. Read and approved the final manuscript: CZ NL MH GC JZ GY XL YH JL YY.

References

  1. 1. Freedman RB, Hirst TR, Tuite MF (1994) Protein disulphide isomerase building bridges in protein folding. Trends Biochem Sci 19: 331–336.
  2. 2. Fisher G (1994) Peptidyl_prolylcis/trans isomerases and their effectors. Angew Chem Inter Ed Eng l33: 1415–1436.
  3. 3. Wu HM, Wensley E, Bhave (2009) Identification and analysis of genes encoding a novel ER-localised cyclophilin B in wheat potentially involved in storage protein folding. Plant Sci 176: 420–432.
  4. 4. Hayano T, Hirose M, Kikuchi M (1995) Protein disulfide isomerase mutant lacking its isomerase activity accelerates folding in the cell. FEBS Lett 377: 505–511.
  5. 5. Quan H, Fan GB, Wang CC (1995) Independence of the chaperone activity of protein disulfide isomerase from its thioredoxin-like active site. J Biol Chem 270: 17078–17080.
  6. 6. Pihlajaniemi T, Helaakoski T, Tasanen K, Myllyla R, Huhtala ML, et al. (1987) Molecular cloning of the beta-subunit of human prolyl 4-hydroxylase. This subunit and protein disulphide isomerase are products of the same gene. EMBO J 6: 643–649.
  7. 7. Wetterau JR, Combs KA, Spinner SN, Joiner BG (1990) Protein disulfide isomerase is a component of the microsomal triglyceride transfer protein complex. J Biol Chem 265: 9800–9807.
  8. 8. Jacquot JP, Gelhaye E, Rouhier N, Corbier C, Didierjean C, et al. (2002) Thioredoxins and related proteins in photosynthetic organisms: molecular basis for thiol dependent regulation. Biochem Pharmacol 64: 1065–1069.
  9. 9. Houston NL, Fan CZ, Xiang QY, Schulze JM, Jung R, et al. (2005) Phylogenetic analyses identify 10 classes of the protein disulfide isomerase family in plants, including single-domain protein disulfide isomerase-related proteins. Plant Physiol 137: 762–778.
  10. 10. Darby NJ, Kemmink J, Creighton TE (1996) Identifying and characterizing a structural domain of protein disulfide isomerase. Biochem 35: 10517–10528.
  11. 11. Kemmink J, Darby NJ, Dijkstra K, Nilges M, Creighton TE (1997) The folding catalyst protein disulfide isomerase is constructed of active and inactive thioredoxin modules. Curr Biol 7: 239–245.
  12. 12. KlappaP, Ruddock LW, Darby NJ, Freedman RB (1998) The b′ domain provides the principal peptide binding site of protein disulfide isomerase but all domains contribute to binding of misfolded proteins. EMBO J 17: 927–935.
  13. 13. Lucero HA, Kaminer B (1999) The role of calcium on the activity of ER calcistorin/protein disulfide isomerase and the significance of the C-terminal and its calcium binding. A comparison with mammalian protein disulfide isomerase. J Biol Chem 274: 3243–3251.
  14. 14. Denecke J, De Rycke R, Botterman J (1992) Plant and mammalian sorting signals for protein retention in the endoplasmic reticulum contain a conserved epitope. EMBO J 11: 2345–2355.
  15. 15. Sönnichsen B, Füllekrug J, Van PN (1994) Retention and retrieval both mechanisms cooperate to maintain calreticulin in the endoplasmic reticulum. J Cell Sci 107: 2705–2717.
  16. 16. Ferrari DM, Soling HD (1999) The protein disulphide-isomerase family: unravelling a string of folds. J Biol Chem 339: 1–10.
  17. 17. d'Aloisio E, Paolacci AR, Dhanapal AP, Tanzarella OA, Porceddu E, et al. (2010) The protein disulfide isomerase gene family in bread wheat (T. aestivum L.). BMC Plant Biol 10: 101.
  18. 18. Wilkinson B, Gilbert HF (2004) Protein disulfide isomerase. Biochim Biophys Acta 1699: 35–44.
  19. 19. Gruber CW, Cemazar M, Heras B, Martin JL, Craik DJ (2006) Protein disulfide isomerase: The structure of oxidative folding. Trends Biochem Sci 31: 455–464.
  20. 20. Takemoto Y, Couglan SJ, Okita TW, Satoh H, Ogawa M, et al. (2002) The rice mutant esp2 greatly accumulates the glutelin precursor and deletes the protein disulfide isomerase. Plant Physiol 128: 1212–1222.
  21. 21. Han XH, Wang YH, Liu X, Jang L, Ren YL, et al. (2012) The failure to express a protein disulphide isomerase-like protein results in a floury endosperm and an endoplasmic reticulum stress response in rice. J Exp Bot 63: 121–130.
  22. 22. Li CP, Larkins BA (1996) Expression of protein disulfide isomerase is elevated in the endosperm of the maize floury-2 mutant. Plant Mol Biol 30: 873–882.
  23. 23. Goldberg RB, Barker SJ, Perez-Grau L (1989) Regulation of gene expression during plant embryogenesis. Cell 56: 149–160.
  24. 24. Kamauchi S, Wadahama H, Iwasaki K, Nakamoto Y, Nishizawa K, et al. (2008) Molecular cloning and characterization of two soybean protein disulfide isomerases as molecular chaperones for seed storage proteins. FEBS J 275: 2644–2658.
  25. 25. Iwasaki K, Kamauchi S, Wadahama H, Ishimoto M, Kawada T, et al. (2009) Molecular cloning and characterization of soybean protein disulfide isomerase family proteins with nonclassic active center motifs. FEBS J 276: 4130–4141.
  26. 26. Wang HZ, Leonor C, Boavida MR, McCormick S (2008) Truncation of a protein disulfide isomerase, PDIL2-1, delays embryo sac maturation and disrupts pollen tube guidance in Arabidopsis thaliana. Plant Cell 20: 3300–3311.
  27. 27. Ondzighi CA, Christopher DA, Cho EJ, Chang SC, Staehelin LA (2008) Arabidopsis protein disulfide isomerase-5 inhibits cysteine proteases during trafficking to vacuoles before programmed cell death of the endothelium in developing seeds. Plant Cell 20: 2205–2220.
  28. 28. Lu DP, David AC (2006) Immunolocalization of a protein disulfide isomer to Arabidopsis thaliana chloroplasts and association with starch biogenesis. Int J Plant Sci 167: 12.
  29. 29. Somanchi A, Mayfield SP (1999) Nuclear–chloroplast signaling. BMC Plant Biol 2: 404–409.
  30. 30. Lu DP, David AC (2008) Endoplasmic reticulum stress activates the expression of a sub-group of protein disulfide isomerase genes and AtbZIP60 modulates the response in Arabidopsis thaliana. Mol Genet Genomics 280: 199–210.
  31. 31. Liu YH, Wang XT, Shi YS, Huang YQ, Song YC, et al. (2009) Expression and characterization of protein disulfide isomerases in maize (Zea mays L.). Chinese J Biochem Mol Biol 25: 229–234.
  32. 32. Han HC, Khurana N, Tyagi AK, Khurana JP, Khurana P (2011) Identification and characterization of high temperature stress responsive genes in bread wheat (Triticum aestivum L.) and their regulation at various stages of development. Plant Mol Biol 75: 35–51.
  33. 33. Ellgaard L, Ruddock LW (2005) The human protein disulphide isomerase family: substrate interactions and functional properties. EMBO Rep 6: 28–32.
  34. 34. Tian G, Xiang S, Noiva R, Lennarz WJ, Schindelin H (2006) The crystal structure of yeast protein disulfide isomerase suggests cooperativity between its active sites. Cell 124: 61–73.
  35. 35. Gruber CW, Cemazar M, Heras B, Martin JL, Craik DJ (2006) Protein disulfide isomerase: the structure of oxidative folding. Trends Biochem Sci 31: 8.
  36. 36. Somanchi A, Mayfield SP (1999) Nuclear–chloroplast signalling. BMC Plant Biol 2: 404–409.
  37. 37. Levitan A, Trebitsh T, Kiss V, Pereg Y, Dangoor I, et al. (2005) Dual targeting of the protein disulphide isomerase RB60 to the chloroplast and the endoplasmic reticulum. Proc Natl Acad Sci 102: 6225–6230.
  38. 38. Monnat J, Neuhaus EM, Pop MS, Ferrari DM, Kramer B, et al. (2000) Identification of a novel saturable endoplasmic reticulum localization mechanism mediated by the C-terminus of a Dictyostelium protein disulfide isomerase. Mol Biol Cell 11: 3469–3484.
  39. 39. Breuza L, Halbeisen R, Jeno P, Otte S, Barlowe C, et al. (2004) Proteomics of endoplasmic reticulum-Golgi intermediate compartment (ERGIC) membranes from Brefeldin A-treated HepG2 cells identifies ERGIC-32, a new cycling protein that interacts with human Erv46. J Biol Chem 279: 47242–47253.
  40. 40. Welsh LM, Tong AHY, Boone C, Jensen ON, Otte S (2006) Genetic and molecular interactions of the Erv41p-Erv46p complex involved in transport between the endoplasmic reticulum and Golgi complex. J Cell Sci 119: 4730–4740.
  41. 41. Shimoni Y, Zhu XZ, Levanony H, Segal G, Galili G (1995) Purification, characterization, and intracellular localization of clycosylated protein disulfide isomerase from wheat grains. Plant Physiol 108: 327–335.
  42. 42. Shimoni Y, Segal G, Zhu XZ, Galili G (1995) Nucleotide sequence of a wheat cDNA encoding protein disulfide isomerase. Plant Physiol 107: 281.
  43. 43. Hermsen R, Tans S, Wolde PR (2006) Transcriptional regulation by competing transcription factor modules. PLoS Comput Biol 2: 164.
  44. 44. Ravel C, Martre P, Romeuf I, Dardevet M, El-Malki R, et al. (2009) Nucleotide polymorphism in the wheat transcriptional activator Spa influences its pattern of expression and has pleiotropic effects on grain protein composition, dough viscoelasticity, and grain hardness. Plant Physiol 151: 2133–2144.
  45. 45. Yamamoto MP, Onodera Y, Touno SM, Takaiwa F (2006) Synergism between RPBF Dof and RISBZ1bZIP activators in the regulation of rice seed expression genes. Plant Physiol 141: 1694–1707.
  46. 46. Yousefi M, Nematzadeh GA, Askari H, Nasiri N (2012) Bioinformatics analysis of promoters Cis-elements and study on genes co-expression of oxidative defense pathway in Oryza sativa L. Plant. Intl J Agric Crop Sci 4: 1240–1245.
  47. 47. Clissold PM, Bicknell R (2003) The thioredoxin-like fold: hidden domains in protein disulfide isomerases and other chaperone proteins. Funct genomics Bioinformatics 25: 603–611.
  48. 48. The International Brachypodium Initiative (2010) Genome sequencing and analysis of themodel grass Brachypodium distachyon. Nature 463: 763–768.
  49. 49. Larré C, Penninck S, Bouchet B, Lollier V, Tranquet O, et al. (2010) Brachypodium distachyon grain: identification and subcellular localization of storage proteins. J Exp Bot 61: 1771–1783.
  50. 50. Laudencia-Chingcuanco DL, Vensel WH (2008) Globulins are the main seed storage proteins in Brachypodium distachyon. Theor Appl Genet 117: 555–563.
  51. 51. Wang K, Han CF, Dong K, Gao LY, Li HY, et al. (2010) Characterization of seed proteome in Brachypodium distachyon. J Cereal Sci 52: 177–186.
  52. 52. Wang S, Wang K, Chen G, Lv D, Han X, et al. (2012) Molecular characterization of LMW-GS genes in Brachypodium distachyon L. reveals highly conserved Glu-3 loci in Triticum and related species. BMC Plant Biol 12: 221.
  53. 53. Guillon F, Larre C, Petipas F, Berger A, Moussawi J, et al. (2012) A comprehensive overview of grain development in Brachypodium distachyon variety Bd21. J Exp Bot 63: 739–755.
  54. 54. Wadahama H, Kamauchi S, Ishimoto M, Kawada T, Urade R (2007) Protein disulfide isomerase family proteins involved in soybean protein biogenesis. FEBS J 274: 687–703.
  55. 55. Wang SL, Yu ZT, Cao M, Shen XX, Li N, et al. (2012) Molecular mechanisms of HMW glutenin subunits from 1Sl genome of Aegilops longissima positively affecting wheat bread making quality. PLoS ONE 8: 58947.
  56. 56. Liu JX, Howell SH (2010) Endoplasmic reticulum protein quality control and its relationship to environmental stress responses in plants. Plant Cell 22: 2930–2942.
  57. 57. Urade R (2007) Cellular response to unfolded proteins in the endoplasmic reticulum of plants. FEBS J 274: 1152–1171.
  58. 58. Mittler R, Vanderauwera S, Gollery M, Van Breusegem F (2004) The reactive oxygen gene network of plants. Trends Plant Sci 9: 490–498.
  59. 59. Sakamoto H, Matsuda O, Iba K (2008) ITN1, a novel gene encoding an ankyrin-repeat protein that affects the ABA-mediated production of reactive oxygen species and is involved in salt-stress tolerance in Arabidopsis thaliana. Plant J 56: 411–422.
  60. 60. Levine A, Pennell RI, Alvarez ME, Palmer R, Lamb C (1996) Calcium-mediated apoptosis in a plant hypersensitive disease resistance response. Curr Biol 6: 427–437.
  61. 61. Gilbert , Hiram F (1997) Protein disulfide isomerase and assisted protein folding. J Biol Chem 272: 29399–29402.
  62. 62. Desikan R, Reynolds A, Hancock JT, Neill SJ (1998) Harpin and hydrogen peroxide both initiate programmed cell death but have differential effects on defense gene expression in Arabidopsis suspension cultures. Biochem J 330: 115–120.
  63. 63. Jabs T, Dietrich RA, Dangl JL (1996) Initiation of runaway cell death in an Arabidopsis mutant by extracellular superoxide. Science 273: 1853–1856.
  64. 64. Bowne JB, Erwin TA, Juttner J, Schnurbusch T, Langridge P, et al. (2012) Drought responses of leaf tissues from wheat cultivars of differing drought tolerance at the metabolite Level. Mol Plant 5: 418–429.
  65. 65. Verelst W, Bertolini E, De Bodt S, Vandepoele K, Demeulenaere M, et al. (2013) Molecular and physiological analysis of growth-limiting drought stress in Brachypodium distachyon leaves. Mol Plant 6: 311–322.
  66. 66. Kim DY, Hong MJ, Jang JH, Seo YW (2012) cDNA-AFLP analysis reveals differential gene expression in response to salt stress in Brachypodium distachyon. Genes Genom 34: 475–484.
  67. 67. Bateman A, Birney E, Cerruti L, Durbin R, Etwiller L, et al. (2002) The Pfam protein families database. Nucleic Acids Res 30: 276–280.
  68. 68. Livak KJ, Schmittgen TD (2001) Analysis of relative gene expression data using real-time quantitative PCR and the 2−ΔΔCT method. Methods 25: 402–408.
  69. 69. Hong SY, Seo PJ, Yang MS, Xiang F, Park CM (2008) Exploring valid reference genes for gene expression studies in Brachypodium distachyon by real-time PCR. BMC Plant Biol 8: 112.