Impact Factor 4.402 | CiteScore 7.8
More on impact ›

Original Research ARTICLE

Front. Plant Sci., 14 June 2017 |

Molecular Characterization, Gene Evolution, and Expression Analysis of the Fructose-1, 6-bisphosphate Aldolase (FBA) Gene Family in Wheat (Triticum aestivum L.)

Geng-Yin Lv1, Xiao-Guang Guo1, Li-Ping Xie1, Chang-Gen Xie1,2, Xiao-Hong Zhang1, Yuan Yang1, Lei Xiao1, Yu-Ying Tang1, Xing-Lai Pan3, Ai-Guang Guo1,2 and Hong Xu1,2*
  • 1College of Life Sciences, Northwest A & F University, Yangling, China
  • 2State Key Laboratory of Crop Stress Biology for Arid Areas, Yangling, China
  • 3Department of Food Crop Science, Cotton Research Institute, Shanxi Academy of Agricultural Sciences (CAAS), Yuncheng, China

Fructose-1, 6-bisphosphate aldolase (FBA) is a key plant enzyme that is involved in glycolysis, gluconeogenesis, and the Calvin cycle. It plays significant roles in biotic and abiotic stress responses, as well as in regulating growth and development processes. In the present paper, 21 genes encoding TaFBA isoenzymes were identified, characterized, and categorized into three groups: class I chloroplast/plastid FBA (CpFBA), class I cytosol FBA (cFBA), and class II chloroplast/plastid FBA. By using a prediction online database and genomic PCR analysis of Chinese Spring nulli-tetrasomic lines, we have confirmed the chromosomal location of these genes in 12 chromosomes of four homologous groups. Sequence and genomic structure analysis revealed the high identity of the allelic TaFBA genes and the origin of different TaFBA genes. Numerous putative environment stimulus-responsive cis-elements have been identified in 1,500-bp regions of TaFBA gene promoters, of which the most abundant are the light-regulated elements (LREs). Phylogenetic reconstruction using the deduced protein sequence of 245 FBA genes indicated an independent evolutionary pathway for the class I and class II groups. Although, earlier studies have indicated that class II FBA only occurs in prokaryote and fungi, our results have demonstrated that a few class II CpFBAs exist in wheat and other closely related species. Class I TaFBA was predicted to be tetramers and class II to be dimers. Gene expression analysis based on microarray and transcriptome databases suggested the distinct role of TaFBAs in different tissues and developmental stages. The TaFBA 4–9 genes were highly expressed in leaves and might play important roles in wheat development. The differential expression patterns of the TaFBA genes in light/dark and a few abiotic stress conditions were also analyzed. The results suggested that LRE cis-elements of TaFBA gene promoters were not directly related to light responses. Most TaFBA genes had higher expression levels in the roots than in the shoots when under various stresses. Class I cytosol TaFBA genes, particularly TaFBA10/12/18 and TaFBA13/16, and three class II TaFBA genes are involved in responses to various abiotic stresses. Class I CpFBA genes in wheat are apparently sensitive to different stress conditions.


Fructose-1,6-bisphosphate aldolase (EC, FBA, or FBPA), also known as aldolase (ALD), is a key metabolic enzyme that catalyzes the reversible aldol cleavage of fructose-1,6- bisphosphate (FBP) into dihydroxyacetone phosphate (DHAP) and glyceraldehyde-3-phosphate (GAP), either in glycolysis or gluconeogenesis and in the Calvin-Benson cycle (Rutter, 1964; Ronimus and Morgan, 2003; Berg et al., 2010). These reactions are involved in carbon fixation and sucrose metabolism and are present in the chloroplast stroma and in the cytosol of green plants (Anderson et al., 2005).

FBAs could be classified into two groups based on different catalytic mechanisms and independent occurrences in evolution (Rutter, 1964; Flechner et al., 1999). Class I FBAs are not inhibited by ethylene diamine tetraacetic acid (EDTA) or affected by potassium ions, and occur in some bacteria, archaea, higher plants, and animals (Penhoet et al., 1967; Tolan et al., 1987). Class II FBAs are inhibited by EDTA (Gross and Al, 1999) and are found in Giardia lamblia, most bacteria, fungi, and yeast (Marsh and Lebherz, 1992; Henze et al., 1998). Some non-green algae (e.g., Cyanophora paradoxa), which is a phylogenetically diverse group, have either class I or class II aldolases or both (Gross et al., 1994; Antia, 2007). Class I FBAs are commonly homotetramers (Perham, 1990; Lorentzen et al., 2004); these activate their donor substrate by forming an intermediate Schiff base with the ÃĆÂęÅ-amino group of a conserved lysine residue (Lebherz and Rutter, 1969; Plaumann et al., 1997). Class II FBAs are dimers, which may use divalent metal cations (mostly Zn2+, Fe2+, or Co2+) to activate their donor homologs, and they belong to the family of (β/α)8 TIM barrel enzymes (Lorentzen et al., 2003; Du et al., 2011). Class II enzymes are divided into subgroups “A” and “B,” depending on their amino acid sequences (Sánchez et al., 2002). Type A aldolases are zinc-dependent and participate in glycolysis and gluconeogenesis, whereas type B aldolases have different divalent metal cofactors and diverse metabolic roles and substrate specificities (Sauvé and Sygusch, 2001; Labbé et al., 2011).

In higher plants, both the cytosolic FBA (cFBA) and chloroplast/plastid FBA (CpFBA) belong to the class I-type of isoenzymes (Anderson and Advani, 1970; Krüger and Schnarrenberger, 1983; Lebherz et al., 1984). These proteins play a vital role in carbohydrate metabolism (Anderson et al., 1995) and in signal transduction (Cho and Yoo, 2011). CpFBA are bifunctional for the formation of fructose-1, 6-bisphosphate (FBP) and sedoheptulose-1,7- bisphosphate (SuBP) in the Calvin cycle (Flechner et al., 1999), as well as function as a sedoheptulose/fructose-bisphosphate aldolase (SFBA) (Peltier et al., 2006). FBP aldolase activity is also part of the glycolytic and gluconeogenic reaction sequence in the cytoplasm, whereas the function of SuBP aldolase in plants is limited to the Calvin cycle that occurs in plastids (Flechner et al., 1999).

Different members of the FBA gene family have been identified and characterized in various plant species, including maize (Dennis et al., 1988), Arabidopsis (Lu et al., 2012), rice (Kagaya et al., 1995), spinach (Pelzer-Reith et al., 1993), tobacco (Yamada et al., 2000), Sesuvium portulacastrum (Fan et al., 2009), and tomato (Cai et al., 2016). FBA genes have been shown to be involved in various important physiological and biochemical processes, e.g., plant development (Zhang et al., 2014), signal transduction (Oelze et al., 2014), regulation of secondary metabolism (Zeng et al., 2014), plant defense and response to biotic (Mohapatra and Mittra, 2016), and abiotic stresses, including salt (Lu et al., 2012), cadmium (Sarry et al., 2006), drought (Khanna et al., 2014), chilling (Purev et al., 2008), and heat (Michelis and Gepstein, 2000), and post-translational modification (Mininno et al., 2012). Furthermore, the presence of FBAs in the nucleus implies that aldose isoenzymes could bind to DNA and directly regulate gene expression (Páez-Valencia et al., 2008).

Common wheat (Triticum aestivum L.) is a hexaploid species (6× = 2n = 42, AABBDD) that originated from two inter-specific hybridizations that are estimated to have taken place ~0.5 million and 10,000 years ago (Dubcovsky and Dvorak, 2007). Its predicted most closely related extant diploid species (2n = 14) include Triticum monococcum or T. urartu (donors for A genome), Aegilops speltoides (S genome related to the B genome), and A.tauschii (D genome). The hexaploid genome of wheat has three homeologous sets of seven pairs of chromosomes (1A to 7A, 1B to 7B, and 1D to 7D), each carrying highly similar gene copies (Choulet et al., 2014).

Despite extensive studies on the FBA genes in various plant species, our understanding of its function in wheat remains unclear. A previous study has revealed that CpFBA accounts for 86% of the total aldolase activity in wheat leaves (Schnarrenberger and Krüger, 1986), and wheat FBA genes could be activated by various abiotic stresses (Xue et al., 2008). FBA has also been linked to male sterility (Li et al., 2012). Consequently, in-depth research investigations on the FBA genes of wheat may provide insights on methods in modifying photosynthesis in increase crop yield.

In the present study, 21 members of the FBA gene family in wheat were identified and cloned. We investigated the molecular characteristics, chromosomal location, gene evolution, protein structures, and expression patterns of these genes. Genome-wide identification, phylogenetic structural and functional analysis revealed the role of the FBA gene family in wheat, which subsequently may be applied to crop production and improvement.

Materials and Methods

Identification of FBA Genes

A total of 21 FBA genes from Triticum aestivum L. (TaFBA) were identified by BLAST analysis against the URGI ( and Ensembl Plants ( databases using the gene sequences of previously annotated FBA genes in wheat (GenBank No. FJ403591.1, AJ420778.1, FJ625793.3, KR139996.1, KR139997.1) and Arabidopsis (GenBank No: AT2G21330, At4G38970, AT2G01140, AT5G03690, AT4G26530, AT2G36460, AT4G26520, AT3G52930, AT1G18270) with E-value < 1e−10. Using these 21 TaFBA genes as queries, another 31 FBA genes from T. monococcum (6 genes), T. urartu (7 genes), A. speltoides (5 genes), A. sharonensis (6 genes), and A. tauschii (7 genes) were further identified from the URGI database. Using the genome sequences of these FBA genes downloaded from the URGI database as queries, the FBA cDNA sequences of T. aestivum, T. urartu, A. sharonensis, and A. tauschii were obtained from the WheatExp database ( and NCBI's TSA and SRA databases. The FBA cDNA sequences of T. monococcum and A. speltoides were predicted by homology analysis.

Chromosomal Localization of Wheat FBA Gene Family

We used URGI, Ensembl Plants databases, wheat_2014_90K SNP gene chip, and Chinese Spring_Deletion gene chip to predict the chromosomal localization of the TaFBA genes. To further confirm our results, gDNA PCR amplification of 21 nulli-tetrasomic lines (NA-TD, NB-TD, and ND-TB) of T. aestivum L.var. Chinese Spring was performed. The gene-specific primers used in PCR analysis are listed in Table S2. Nulli-tetrasomic Chinese Spring genotypes contain four copies of one chromosome pair (tetrasomic) to compensate for the lack of a homoeologous chromosome pair (nullisomic) (Sears et al., 1966). For instance, Nulli1A-Tetra1D (N1AT1D) lacks chromosome 1A (nullisomic-1A), but contains two chromosome pairs of chromosome 1D (tetrasomic-1D), resulting in a line containing no copies of chromosome 1A, two doses of chromosome 1B, and four doses of chromosome 1D. PCR analysis of genomic DNA from nulli-tetrasomic lines allows one to determine which chromosome gene is located on based on failure to amplify specific nullisomic lines (Ohnishi et al., 2008). PCR amplification was performed as follows: 94°C for 5 min; 94°C for 30 s, annealing at 60°C for 30 s, and extension at 72°C for 1 min, 35 cycles; and 72°C for 10 min for the final extension. PCR reactions were performed using the proofreading enzymes LA Taq or PrimeSTAR® HS DNA Polymerase (TaKaRa, Japan) depending on the application.

DNA Cloning and Sequence Alignment

21 TaFBA genes (including 1.5-kb promoter regions) were cloned by genomic PCR of T. aestivum L. var. Chinese Spring. PCR protocols were the same as that used in chromosomal localization described in 2.2. The promoter sequences of two TaFBA genes (TaFBA6 and TaFBA12) were obtained by high-efficiency thermal asymmetric interlaced PCR (hiTAIL-PCR) (Liu and Chen, 2007) due to the incomplete sequencing of the wheat genome. The primers used in this study are listed in Table S2. The PCR products were purified using an AxyPrep DNA gel extraction kit (Axygen, USA) and ligated into the pMD19-T vector (TaKaRa, Japan). The recombinant plasmid DNA clones were sequenced by Invitrogen (USA). The generated TaFBA gene sequences were then submitted to GenBank of NCBI (Accession No. were listed in Table 1).


Table 1. The molecular characteristics of TaFBA genes and the prediction of chromosomal and subcellular location.

Multiple sequences alignment of 21 TaFBA genes and 31 FBA genes from wheat relatives were performed by MUSCLE ( A rooted UPGMA phylogenetic tree was constructed with MEGA 6 under default parameters and bootstrapping with 1,000 replicates (Tamura et al., 2011). Genome sequences, cDNA sequences and protein primary sequences of FBAs were aligned by DNAMAN 6.0 software with pairwise method and were clustered by MeV 4.9 using the average linkage hierarchical clustering (HCL) method.

Annotation of TaFBA Gene Structures and Cis-Regulatory Elements in the Promoter Region

The exon-intron structure of TaFBA genes was determined by aligning the cDNA sequences to the corresponding genomic sequences using Gene Structure Display Server (GSDS, The transposable elements of TaFBA genes were predicted on TREP ( and LTR_FINDER ( Putative cis-acting regulatory DNA elements in the promoter sequences (1.5-kb upstream of the 5′-UTR) of TaFBA genes were annotated with PlantCARE (, and displayed in Argo Genome Browser v1.0.31 ( The exon-intron structure of the TaFBA genes was determined by aligning the cDNA sequences to the corresponding genomic sequences using the Gene Structure Display Server (GSDS, The transposable elements of the TaFBA genes were predicted by using TREP ( and LTR_FINDER ( Putative cis-acting regulatory DNA elements in the promoter region (1.5-kb upstream of the 5'-UTR) of the TaFBA genes were annotated with PlantCARE ( and displayed in the Argo Genome Browser v1.0.31 (

The Primary Structure and Three-Dimensional (3D) Structure Prediction of the FBA Proteins

The physicochemical characteristics of the protein sequence of each FBA such as the number of amino acids (aa), molecular weight (MW), isoelectric point (pI), and grand average of hydropathy (GRAVY) value were calculated with the ProtParam tool in ExPASy ( The subcellular location of each FBA was predicted by using WoLF PSORT (Horton et al., 2007). Functional domains and conserved motifs were annotated with the Pfam database (Finn et al., 2016) and the MEME website (

A total of 245 FBA proteins of archaea, bacteria, and eukaryotes were identified by PHMMER searches on the Ensembl Plants database and key word searches of “fructose-1,6-bisphosphate aldolase” in the UniprotKB/Swiss-Prot databases. HMMER 3.0 was employed to perform an HMM search (Zhang and Wood, 2003), with the family-specific Glycolytic (PF00274) and F_bP_aldolase domain (PF01116).

Amino acid sequence alignment of the FBAs was performed by using the Clustal Omega method (Sievers et al., 2011), and a rooted maximum likelihood (ML) phylogenetic tree was constructed using MEGA 6. The phylogenetic tree files were edited by Evolview ( We used the I-TASSER program (Zhang, 2008) and Swiss-PdbViewer v4.1.0 (Schwede et al., 2003) to remodel and analyze the tertiary structure, and SWISS-MODEL to construct the quaternary structure of the TaFBAs.

Gene Expression Profile Analysis

To analyze the expression profiles of the TaFBA genes, the microarray data of the TaFBA genes were downloaded from PLEXdb (Dash et al., 2012) and the RNA-seq data from wheat transcriptome database WheatExp. Combined with the analysis using Genevestigator (Hruz et al., 2008), the expression profiles of different tissues and developmental stages of the TaFBA genes were generated by using OriginPro 9.1.

Quantitative Real-Time PCR (qRT-PCR) Analysis of the Response of the TaFBA Genes to Different Abiotic Stresses

Seeds of Chinese Spring were sterilized with 75% alcohol for 30 s and 15% sodium hypochlorite for 5 min, rinsed 5 times, placed on moistened filter paper in Petri dishes, and germinated in the dark for 2 days. Then, the wheat seedlings were cultivated in Hoagland liquid culture medium at 23°C and 16 h light/8 h dark cycles. Treatment of the wheat seedlings was performed as described Zeng et al. (2016), with minor modifications. After 10 days of growth, salinity (200 mM NaCl), drought (15 % PEG 6000), ABA (50 μM ABA), heat (40°C), and cold (4°C) treatments were conducted. The shoots and roots of the seedlings were collected at 0, 1, 2, 6, 12, 24, and 48 h after treatment.

We investigated the influence of light on the expression of the TaFBA genes as described by Zhao et al. (2014). The etiolated wheat seedlings were cultured under continuous light, whereas the normal-cultured seedlings were placed in the dark after being exposure to light for 24 h. Wheat leaves were collected at 1, 2, 4, and 8 h after light or dark treatment, immediately frozen in liquid nitrogen, and kept at −80°C until RNA isolation. Next, total RNA were isolated by using the RNAiso plus reagent (TaKaRa, Japan) and treated with gDNA Eraser (TaKaRa, Japan) for 2 min at 42°C to degrade any residual genomic DNA. Then, first-strand cDNAs were synthesized from the total RNA by using a PrimeScript™ RT reagent kit (TaKaRa, Japan) according to the manufacturer's instructions. Finally, qRT- PCR was performed in optical 96-well plates (VIOX, UK) with a CFX96 Touch Real-Time PCR Detection System (BIO-RAD, USA) by using the SYBR Green method. The wheat ADP ribosylation factor (ADP-RF) gene was used as reference gene (Paolacci et al., 2009) to normalize the expression data. The thermal cycle protocol was set up as follows: 95°C for 30 s; 95°C for 5 s, and 60°C for 30 s for 40 cycles. The gene specific primers used for qRT-PCR were listed in Table S8. The quantitative analysis was accomplished with the 2−ΔΔCT method. PCR was performed based on three technical replicates for each of the biological duplicates.


Genome-Wide Identification and Chromosomal Localization of the FBA Genes in Wheat

To investigate the TaFBA gene families, BLAST analysis with FBA genes of wheat and Arabidopsis thaliana (GenBank Accession Nos. are shown in 2.1) was performed using the IWGSC database. A total of 21 TaFBA genes (named as TaFBA1~21) were identified and cloned (Data sheet DOC1, TXT2). The cDNA sequences (Data Sheet TXT1) were obtained from NCBI and the WheatExp Database.

We aligned the cDNA and predicted protein sequences of the TaFBA genes by using DNAMAN with the pairwise method (Table S1). Phylogenetic and sequence analyses revealed that the TaFBA genes could be classified into two subfamilies, classes I and II. There were 18 TaFBA genes in class I, with TaFBA1~3, TaFBA4~6, TaFBA7~9, and TaFBA10~16 showing high identity (>90%) respectively. Meanwhile, three class II TaFBA genes (TaFBA19~21) were highly homologous and showed lower identity (< 30%) with those of class I.

The molecular characteristics of the TaFBA genes and their subcellular location are listed in Table 1. The predicted MW of class I TaFBA proteins ranged from 25.93 to 55.39 kDa, with TaFBA17 apparently being the smallest polypeptide, whereas class II TaFBAs were about 148 kDa, bigger than class I. WoLF PSORT was used to predict the subcellular location of 21 putative TaFBA proteins. Similar to Arabidopsis, rice, and tomato, 18 class I TaFBAs were located in two compartments: TaFBA1~9 were in the chloroplast/plastid and were thus designated as CpFBAs, whereas TaFBA10~18 were localized to the cytoplasm, and hereby named as cFBA. Three class II proteins TaFBA19~21 might also be located in the chloroplast/plastid, and thus described as CpFBAs.

Chromosomal Location of the FBA Genes in Wheat

Based on the 0.6× Chinese Spring genome draft sequence (Mayer et al., 2014), we predicted the chromosomal location of the TaFBA genes (Table 1). In addition, the TaFBA genes were queried on the mapped loci using EST-derived probes in GrainGenes-SQL databases. Therefore, the TaFBA1, 2, 3, 4, 7, 8, 11, 19, and 20 genes were mapped onto different gene loci through a wheat_2014_90K SNP gene chip (Figure S1A), and the TaFBA10, 12, 14, and 15 genes were mapped using a Chinese Spring_Deletion gene chip (Figure S1B).

To confirm the chromosomal location and identify the primer specificity of TaFBA genes, 21 Chinese Spring nulli-tetrasomic lines were used to amplify genomic DNA (The gene -specific primers used are listed in Table S2). The PCR results (Figure 1) confirmed the location of each TaFBA gene copy, as indicated by the failed amplification in the specific nulli-tetrasomic line. These findings validated that the genes were located within the same locus as predicted in Table 1 and Figure S1.


Figure 1. Genomic PCR amplification results of the TaFBA genes using Chinese spring nulli-tetrasomic lines. PCR amplification was performed using Chinese Spring (CS) and nulli-tetrasomic lines of Chinese Spring (N4-T4) genomic DNA. DL5000 is DNA marker (100, 250, 500, 750, 1,000, 1,500, 2,000, 3,000, 5,000 bp). The white arrows indicated the target PCR bands.

A total of 21 TaFBA genes were localized to 12 chromosomes of 4 homoeologous groups: TaFBA1~3 genes in the short arms and TaFBA10~16 in the long arms of homoeologous group 3; the TaFBA5/6 genes in the short arm, and TaFBA4 in the long arm of homoeologous group 4; the TaFBA7~9 and TaFBA17/18 genes in the short arms of homoeologous group 5; and the TaFBA19~21 genes located in the short arms of homoeologous group 7.

Phylogenetic Analysis of the FBA Genes

For the investigation of the molecular evolution of the TaFBA gene family, 31 FBA genes from other closely related wheat species were identified: six TmFBA genes from T. monococcum (AmAm), seven TuFBA genes from T. urartu (AuAu), five AspFBA genes from A. speltoides (SS), six AshFBA genes from A. sharonensis (SshSsh), and seven AtaFBA genes from A. tauschii (DD). The gene IDs and sequences are listed in Table S3, and Data Sheets TXT4, TXT 5. Then, an unrooted phylogenetic tree was constructed using MUSCLE in MEGA6 (Figure 2), and pairwise alignments were conducted using the hierarchical clustering method by MeV (Figure S2).


Figure 2. Exon–intron organization and the phylogenetic analysis of the FBA gene families in wheat and wheat relatives. Gene structures of FBAs analysed by GSDS. Exons are shown as Double-sided wedges, and different colours indicate different FBA gene groups. Introns are shown as thin lines. Untranslated regions (UTRs) are shown as blank boxes. The exon and intron sizes can be estimated using the scale at the bottom. TaFBA, TmFBA, TuFBA, AspFBA, AshFBA, AtaFBA indicated the FBA genes from T. Aestivum, T. monococcum, T. urartu, A. speltoides, A. Sharonensis, A. tauschii respectively. The unrooted tree was generated using MUSCLE in MEGA6.

Owing to the transcript annotation of the wheat genome, the analysis and comparison of the structural features of the FBAs in different subfamilies were also conducted (Figure 2). The organization (number, order, and length) of the exons were mostly conserved within different FBA groups, whereas the introns and UTRs showed variable lengths and distribution. Based on the exon numbers and intron lengths, a total of 52 FBA genes from wheat and other closely related species could be divided into six independent subgroups: class Ia ~ class Ie and class II. 21 TaFBA genes belonged to different subgroups: TaFBA7/8/9 genes in class Ia, TaFBA4/5/6 genes in class Ib, TaFBA1/2/3 genes in class Ic, TaFBA10/12/15/17/18 genes in class Id, TaFBA11/13/14/16 genes in class Ie, and TaFBA19/20/21 genes in class II. Each subgroup contained five wheat relative FBA genes, except for six in class Ie. Class II FBA genes existed in both wheat and its closely related species.

Various patterns of exon-intron architecture were identified. For instance, class Ia genes and most cytoplasmic TaFBA genes had one intron, and class Ib and class Ic genes had five introns. On the other hand, class II TaFBA genes contained 41 introns because of the integration of F_bP_aldolase domain and other functional domains. Generally, a higher number of introns could cause alternative splicing and different splice variants, and regulate gene expression at the posttranscriptional level. Whether there are different transcripts of class II genes is thus worth exploring further.

In addition, the annotation of genome sequences suggested that different kinds of transposable elements (TEs) were distributed unevenly in the promoter and intron regions of the TaFBA genomes (Figure S3, Table S4) such as long terminal repeats (LTRs), short interspersed nuclear elements (SINEs), terminal inverted repeats (TIRs), and other TEs. Several TEs were detected in the TaFBA19 and TaFBA20 intron regions, which might influence RNA splicing.

Evolutionary Analysis of FBA Proteins

Using HMMER 3.0, a Uniprot KB/Swiss-Prot database search was performed using the query “fructose 1,6-bisphosphate aldolase,” and 211 sequences from different species were downloaded for FBA protein evolutionary analysis. Approximately 23 of these sequences were removed by pairwise comparison and the absence of complete adolase-type TIM domain. Together with plant FBA protein sequences identified by PHMMER from EnsemblPlants database, a total of 245 FBA proteins were obtained, which consisted of 19 archaeal FBAs, 97 bacterial FBAs, and 129 eukaryotic FBAs (listed in Table S5, Data Sheets TXT3, TXT6). Multiple primary sequences of FBA protein were aligned by using Clustal Omega, and a rooted ML phylogenetic tree was constructed by using MEGA6 with default parameters (Figure 3).


Figure 3. Phylogenetic and structure analysis of the FBA proteins. (A) The phylogenetic tree of FBA proteins constructed with Clustal Omega. Class I and class II FBA subfamilies are distinguished by blue and red colours respectively. with the full-length amino acid sequences of the 245 FBA proteins. 19 archaea FBAs are indicated by orange branches. 97 bacteria FBAs are indicated by blue branches. 129 eukaryota FBAs are indicated by purple branches. Red circle represents bilaterian. Green circle represents viridiplantae. Crimson circle represents chlamydia. Black circle represents Dictyostelium discoideum. Gold circle represents Euryarchaeota. Orchid circle represents fungi. Orange circle represents Plasmodium. Chartreuse circle represents Porphyromonas gingivalis. DarkMagenta circle represents Proteobacteria. Magenta circle represents Spirochaetales. Blue circle represents TACK group. Pink circle represents terrabacteria group. 21 TaFBAs were shown by little red circle. The annulus next to the tree represents the protein domains of FBAs and the outside annulus represents the MEME motifs. (B) Motif LOGOs of FBA proteins generated by MEME.

Evolutionary analysis revealed that the FBAs in various species were clearly classified into two groups, namely, classes I and II (Figure 3A). The class I FBAs in plants were classified into two subgroups, class I cFBAs, and class I CpFBA, occurring in plastids and the cytoplasm, respectively. The class I cFBAs in plants were more closely related to the FBAs in animals than class I CpFBAs. There were two subgroups (types A and B) in class II FBAs. Most FBAs in fungi belonged to type A, and 10 FBAs in plants (including TaFBA19~21) belonged to type B. Both plant cFBAs and CpFBAs were more distantly related to the FBAs in bacteria and fungi.

To investigate the conserved domain and residues of TaFBA proteins, we aligned the wheat FBA protein sequences and conserved sites by using Pfam and MEME. A total of 8 conserved protein domains and 30 motifs were defined (Figure 3). Most of the class I FBAs possessed a glycolytic protein domain, and the other class I FBAs possessed a DeoC (deoxyribose-phosphate aldolase) domain. Type A of class II FBAs possessed one F_bP_aldolase domain or FBPase_3 (fructose-1,6-bisphosphatase) domain. All of the type B of class II FBAs possessed an FBPase_3 domain, but the class II FBAs of plants possessed the other 4 domains, including NAD_binding_2 (NAD-binding domain of 6-phosphogluconate dehydrogenase), NAD_binding_11 (NAD-binding of NADP-dependent 3-hydroxyisobutyrate dehydrogenase), DUF1537 (putative sugar-binding N-terminal domain), and DUF1357_C domain (putative nucleotide-binding of sugar-metabolizing enzyme), which suggest that class II FBAs are NADP-dependent and probably participate in sugar sensing and signaling in plants. Several identical regions of plant FBAs were fairly conserved such as “EGTLLKPNMVTPG,” “GARFAKWR,” “LSGGQSEEEA,” “GILAADES,” “LVPIYEPE,” “RALQ,” “ILFEET,” and “RAKANS” for class I FBAs (Figure 3B). Among these regions, the “LSGGQSEEEA” (TIM _phosphate_binding superfamily), “LVPIYEPE,” and “ILFEET” matched well with that of animal/fungi/bacterial FBAs, suggesting that FBAs were highly conserved during evolution.

Higher-Order Structure of the TaFBA Proteins

The quaternary structure of three wheat FBA proteins (TaFBA4, TaFBA10, and TaFBA20) without N-terminal transit peptides were predicted by using SWISS-MODEL and I-TASSER (Figure 4). TaFBA4 and TaFBA10 belong to class I subfamily and could form tetramers based on their relatively high similarity to class I rabbit muscle aldolase (Blom and Sygusch, 1997) and human muscle aldolase (Dalby et al., 1999) respectively. TaFBA20 is a class II protein that is predicted to form dimers based on its similarity to class II aldolases of Thermus aquaticus (Izard and Sygusch, 2004).


Figure 4. Predicted structures of TaFBA protein monomers and homo-oligomers. (A) Monomer TaFBA4. (B) Monomer TaFBA10. (C) Monomer TaFBA20. The C- and N-termini are labeled for monomer. (D) Tetrameric TaFBA4. (E) Tetrameric TaFBA10. (F) Dimeric TaFBA20. (G) Active site residues of TaFBA4. (H) Active site residues of TaFBA10. (I) Active site residues of TaFBA20. For (A–F), Each monomer is colored separately, and A and B interfaces are indicated by arrows. The sites of the Asp126/124 substitutions are indicated on interface B, the C- and the N-termini are labeled for monomer A. The active site residues involved in substrate binding and catalysis are shown in different colours. For (G–I), Lys226/225 (G,H) situated at the centre of the active region responsible for Schiff base formation, the filled circle of represents divalent metal cation in the three open protomers of TaFBA20.

Similar to other tetrameric FBAs, interfaces A and B were observed in the TaFBA4 and TaFBA10 tetramers (Figures 4D,E). In contrast to interface A, which comprised helix-packing interactions, interface B exhibited loop-loop interactions that were formed by buried hydrogen bonds. In TaFBA4, each interface B had six hydrogen bonds that were involved in the carboxylate “O” atoms of Asp126, interacting with the backbone amides of three consecutive residues (G124-L125-D126) (Sherawat et al., 2008) (Figures 4A–C). Different from TaFBA4, interface B of TaFBA10 was related to Asp124, which interacts with G122-F123-D124.

The catalytic residues in the active region of class I FBAs are highly conserved (Maurady et al., 2002). TaFBA4 contained nine catalytic residues, D32-K105-K144-R146-E184-E186-K226-S268-R298. The catalytic residues in TaFBA10 included D30-K103-K142-R144- E183-E185-K225-S266-R298. Although, class I TaFBAs had the same catalytic residue sequences, different conformations in the active sites would affect the spatial structures (Figures 4G,H). Additionally, class II TaFBAs were the same as the FBAs in Thermus aquaticus, which had active sites including imidazole rings of H81, H178, and H210, and the carboxylate of E132, and the sites also acted as divalent metal ion-binding sites (Figure 4I).

The amino acid sequence alignment of the TIM barrel domain (Figure S4) indicated that the active sites of TaFBA1~TaFBA16 (class I) were homologous to those of rabbit and human FBA isozymes, and the active sites among TaFBA19~21 (class II) corresponded to those of FBA isozymes in Thermus aquaticus. A few substitution mutations and deletion sites were observed in TaFBA17 and TaFBA18, and the catalytic active site sequence of TaFBA17 was D-K-T-P-K-S-R, and that of TaFBA18 was D-K-K-R-K-S-R.

Cis-Elements in the TaFBA Gene Promoters

Cis-elements are important molecular switches that are involved in the regulation of gene transcription during plant growth, development, and responses to biotic and abiotic stresses. The 1.5-kb promoter sequences upstream of the 5′-UTR of 19 TaFBA genes (excluded TaFBA19/21) were identified from wheat genome sequences and used in plant cis-acting regulatory elements analysis in the PlantCARE database (Figure 5, Table 2).


Figure 5. Phytohormone- and stress-responsive cis-elements in the promoter regions of TaFBA genes. 15 Putative ABA-responsive elements (ABRE), Auxin-responsive elements (ARE), GA-responsive elements (GARE), Low-temperature responsive elements (LTRE), Light-regulated elements (LRE), Drought-induced elements (DIRE), Ethylene-responsive elements(ERE), Fungal-elicitor responsive elements (FERE), SA-responsive elements (SARE), MeJA-responsive elements (MeJARE), Anaerobically-induced elements (AIRE), Heat-stress responsive elements (HSRE), Sugar-repression responsive elements (SSRE), Wounding-and pathogen-responsive elements (WPRE), and Defense- and stress-responsive elements (DSRE) core sequences in the 1,500-bp promoter regions of TaFBA genes were predicted using Plant CARE. The lines denote promoter sequences. The elements represented by different colours are indicated above the lines.


Table 2. Cis-elements in the promoter region of 19 TaFBA genes.

Various putative environment stimulus-responsive cis-elements were identified (Table S6). Because TaFBA genes mostly possess multiple phytohormone and abiotic stress-responsive elements, we considered that the expression pattern of TaFBA genes could be regulated by various environmental factors. LREs were highly enriched in 18 TaFBA gene promoters. These findings indicate that the TaFBA genes might be involved in light responses.

Expression Profiles of the TaFBA Genes in Different Tissues and Developmental Stages

The expression profiles of different tissues and developmental stages were downloaded from the WheatExp database and PLEXdb database respectively, and the corresponding probe ID of the TaFBA genes are shown in Table S7. Combined with the results of Genevestigator, we analyzed the spatiotemporal expression profiles of the members of the TaFBA gene family (Figure 6).


Figure 6. Expression profiles of TaFBAs in different tissues and different developmental stages. (A) Expression profiles of TaFBA genes in different tissues. (B) Expression profiles of TaFBA genes at different development stages. Number 1–10 indicate: 1-germination, 2-seedling growth, 3-tillering, 4-stem elongation, 5-booting, 6-inflorescence emergence, 7-anthesis, 8- milk, 9-dough, and10- ripening stages respectively.

The expression of the TaFBA genes showed tissue specificity (Figure 6A). TaFBA4-9 (class I CpFBA genes) showed similar expression patterns; these were upregulated in leaves and downregulated in the roots, particularly TaFBA 4 and 5. On the other hand, most class I cFBA genes were apparently upregulated in the roots. TaFBA12 showed significantly higher expression levels in all tissues, particularly in the roots. TaFBA19/20/21 (class II CpFBA genes) were slightly and constantly expressed in all tissues.

The wheat TaFBA genes were expressed at different developmental stages (Figure 6B). The expression level of TaFBA10/12/18 was higher than that of the other genes, whereas that of TaFBA19/20/21 was lower. The expression profiles of TaFBA4/5/6 and TaFBA7/8/9 varied with different developmental stages. Based on the results of differential expression and phylogenetic analyses, the TaFBA genes were classified into eight gene clusters: TaFBA1/2/3, TaFBA4/5/6, TaFBA7/8/9, TaFBA14/15/17, TaFBA10/12/18, TaFBA11, TaFBA13/16, and TaFBA19/20/21.

Responses of TaFBA Genes to Light

Most TaFBA gene promoters were highly enriched with LREs (Figure 5 and Table 2). Thus, the expression patterns of the TaFBA genes under light and dark treatment were investigated by using qRT-PCR (Figure 7). TaFBA1-9 (CpFBA) and TaFBA10/12/18 (cFBA) were downregulated under short-term light treatment (Figure 7A), whereas the other TaFBAs were upregulated. Meanwhile, all TaFBA genes were immediately upregulated within 1 h of transferring from light to dark, especially TaFBA4-9 (Figure 7B). TaFBA14/15/17, TaFBA11, TaFBA13/16, and TaFBA19/20/21 were induced by light, whereas TaFBA4/5/6, TaFBA7/8/9, and TaFBA10/12/18 were induced by short-term exposure to the dark. These results demonstrate that the LRE cis-elements of the TaFBA genes were not directly related to light responses. Therefore, FBA isozymes might play different roles in various biological processes involved in light signal transduction.


Figure 7. Differential expression analysis of TaFBA genes with light/dark treatments. (A) Light treatment. Total RNA was isolated from etiolated two-leaf seedling at 0, 1, 4, and 8 h after exposure to light. (B) Dark treatment. Two-leaf seedlings cultured under 16 h light/8 h dark were used and placed in darkness for 0, 1, 4, and 8 h after 24 h of continuous illumination. The data came from qRT-PCR analysis with 2−ΔΔCt method.

Expression Profiles of the TaFBA Genes under Abiotic Stresses

The expression profiles of TaFBA gene clusters under different conditions (salt, drought, ABA, heat, and low temperature) were detected using qRT-PCR. The results revealed the complicated expression patterns of the TaFBA gene family in response to various abiotic stresses (Figure 8). The gene specific primers used for qRT-PCR are listed in Table S8.


Figure 8. Expression profiles of TaFBA genes in shoots (A) and roots (B) under abiotic stresses. The data came from qRT-PCR analysis with 2−ΔΔCt method. For each of the TaFBA genes, the relative expression value under normal condition was defined as 1.

In shoots (Figure 8A), the class I cytosol TaFBA genes displayed active responses to multiple abiotic stresses. The expression of TaFBA11 and TaFBA13/16 was significantly induced by high temperature. TaFBA14/15/17 and TaFBA10/12/18 were expressed during exposure to drought and ABA. Under salt stress, most TaFBA genes were downregulated except for TaFBA10/12/18. On the other hand, all class I CpFBA genes were apparently sensitive to multiple stresses, as indicated by a repression in expression. On the other hand, class II CpFBA genes TaFBA19/20/21 were induced after short-term exposure to ABA, heat, and low temperature, implying the role of class II TaFBA genes in stress responses.

The expression pattern of TaFBA genes in roots (Figure 8B) was obviously different from shoots. ABA might lead to the similar change as drought to each gene cluster. Both cFBA and CpFBA were induced by drought, ABA, heat and cold, but only cFBA was upregulated by salt. Among cFBA genes, TaFBA10/12/18 were up-regulated in multiple conditions except heat, TaFBA11 and TaFBA13/16 were up-regulated in different stresses except low temperature. In CpFBA genes, TaFBA1/2/3 could be induced by drought and ABA, TaFBA4/5/6 could be induced by drought and heat, and TaFBA19/20/21 could be induced by all stresses, especially by heat and cold.


One key factor in the success of wheat as a global food crop is its adaptability to a wide variety of climatic conditions. This is attributed, in part, to its allohexaploid genome structure, which arose as a result of two polyploidization events (Mayer et al., 2014). In the present study, 21 TaFBA genes were identified in Chinese spring, including 18 class I FBA genes and 3 class II genes. Therefore, in-depth information on the FBA gene family has been annotated only in two plants: wheat and Arabidopsis. There are 8 AtFBA gene members in Arabidopsis (Lu et al., 2012), AtFBA1~3 occur in plastids, whereas AtFBA4~8 has been localized to the cytoplasm.

A total of 21 TaFBA genes have been localized to 12 chromosomes of 4 homoeologous groups, and most TaFBA gene loci have three copies distributed across three genomes of wheat. We have observed that TaFBA4 may be in the wrong location (Chr.4AL instead of Chr.4AS) because of its high identity with the TaFBA5/6 genes (97%). This could have been caused by chromosomal rearrangements, in that the proximal segment of Chr.4AL was co-linear with the proximal segments of Chr.4BS and 4DS (Devos et al., 1995). We believe that whole-genome duplication and segmental duplication may have contributed to the expansion of the TaFBA gene family. Gene duplication not only expands genome content but also diversifies gene function to ensure optimal adaptability and evolution of plants (Xu et al., 2012). Multiple isozymes ensure the essential function of FBA in the Calvin cycle, glycolysis, and gluconeogenesis, as well as lead to gene redundancy.

The TaFBA genes were most closely related to recent progenitors (Figure 2). For example, TaFBA1 (located in Chr.3AS) was more closely related to TmFBA-1 (97.7% identity) and TuFBA-1 (98.1% identity), which corresponded to the hypothesis that T. monococcum and T. urartu may be the A-genome donor relatives (Dvorak et al., 1988; Dubcovsky et al., 1995). In addition, the TaFBA genes on the A and B genomes had higher identity to the allelic genes on the D genome relative to each other. For instance, the TaFBA2 on Chr.3B was more similar to the TaFBA3 on Chr.3D than to the TaFBA1 on Chr.3A, and the TaFBA4 on Chr.4A was more similar to TaFBA6 on Chr.4D than that in Chr.TaFBA5 on 4B (Figure 2). This observation was consistent with models of interline age hybridization in the Triticeae (Escobar et al., 2011; Civáň et al., 2013) and phylogenomics analyses that the D genome is a product of homoploid hybrid speciation between the A and B genome ancestors >5 million years ago (Marcussen et al., 2014; Mayer et al., 2014).

It has been proposed that certain Calvin cycle enzymes also function in glycolysis or gluconeogenesis, thus photosynthetic eukaryotes would be predicted to have cytosol enzymes derived from the eukaryotic host and chloroplast/plastid enzymes from the cyanobacterial endosymbiont (Rogers and Keeling, 2004; Allen et al., 2012). The evolutionary study on plant FBA genes is useful in investigating the origin of chloroplast and photosynthetic genes. Plaumann et al. (1997) reported that class II CpFBAs in Euglena gracilis and ascomycetes originated from eubacteria via endosymbiotic gene transfer. In the present study, we identified three different groups of FBAs in wheat, and each group appeared to have distinct evolutionary origin and function. Phylogenetic analysis (Figure 3) showed that class I CpFBAs in plants are closely related to the proteins of green algae, indicating that class I CpFBAs might have been derived from the endosymbiotic transfer of genes between green algae and its plant eukaryotic host. Class I cytosol FBAs are conserved in animals and plants, indicating that these might have been derived from a eukaryotic host. Class II TaFBAs were homologous to FBAs of bacteria and seemed to be of eubacterial origin. We speculated that class I CpFBAs, class I cFBAs, and class II CpFBAs might have been derived from green algae, eukaryotic hosts, and eubacteria, respectively, which was similar to the findings of Rogers and Keeling (2004) and Willard and Gibbs (1968).

Although, the exact function of each TaFBA gene is unclear, we observed that different subgroups of TaFBA genes have tissue, stage, and stress-response specificity. For instance, TaFBA4/5/6 had more tissue and development specificity than the others, and TaFBA10/12/18 could be induced by all kinds of abiotic stresses. In addition, TaFBA4/5/6 was upregulated in leaf tissues (Figure 6A), might be involved in the regulation of enzyme activities in leaves, and play important regulatory roles during wheat development.

Several research studies on the responses of plant FBA genes to abiotic stress have been reported. Plastid aldose AldP2 is upregulated by salt stress in Nicotiana (Yamada et al., 2000). Abiotic stimuli could rapidly trigger a significant induction of FBA genes in Sesuvium portulacastrum (Fan et al., 2009). An FBA-dependent fructose signaling pathway acts downstream of the abscisic acid pathway in Arabidopsis thaliana (Cho and Yoo, 2011). Class I cFBAs in Medicago sativa has been identified to have an NMH7 MADS domain (Páez-Valencia et al., 2008), and FBA is involved in the control of RNA polymerase III-directed transcription (Cieśla et al., 2014). These results demonstrate that FBA displays an important role in responses to abiotic stress in plants, but the difference between CpFBAs and cFBAs is unkown.

In the present study, we investigated the responses of wheat FBA genes family to salt, drought, ABA, heat, and low temperature. The results indicate that most TaFBA genes in the roots showed higher expression levels than in shoots under abiotic conditions. Most cytosol TaFBA genes, especially TaFBA10/12/18 and TaFBA13/16, could be induced by abiotic stresses, whereas most class I CpFBAs in wheat might be sensitive to stress conditions. Furthermore, the expression level of class II gene TaFBA19/20/21 was immediately upregulated under stresses in both roots and shoots. These results suggest that cytosolic TaFBAs and class II TaFBA genes could play important roles in the responses to abiotic stresses, which coincided with the findings of previous studies. We plan to conduct additional experiments to investigate the molecular mechanism underlying TaFBA biofunction.

The FBA of the Benson-Calvin cycle is not identical to the analogous enzymes of the Embden-Meyerhof-Parnas pathway, and there exists no cross-reactivity between the cytosol and chloroplast aldolase (Krüger and Schnarrenberger, 1983). Each member of the FBA gene family might thus have different biochemical activity. TaFBA4/5/6 and TaFBA7/8/9 genes (Class I CpFBA) could be induced by short-term exposure to darkness and repressed by photostimulation, but TaFBA14/15/17, TaFBA11, and TaFBA13/16 genes (Class I cFBA) showed the contrary response to light/dark (Figure 7). The discrepancies in expression profiles are indicative of the multiple functions of different TaFBA genes, and FBAs might play a more complicated role in the regulation of glycolysis and carbon concentration. According to the predicted protein structure, the active sites of dimeric class II FBAs also serve as the divalent metal cation-binding sites (Figure 4). Under light irradiation, photosynthesis induces the production of NADPH, and the light-stimulated H+ shift is countered by Mg2+ and other cations moving from thylakoids to stroma, which in turn activate chloroplast class II FBAs. Hence, we considered that class II FBAs are more active in the Calvin cycle.

Different sugar signals generated by photosynthesis and carbon metabolism in light/dark condition might modulate multiple HXK-dependent and HXK-independent pathways and could regulate transcription, translation, protein stability, and enzymatic activity (Rolland et al., 2006), and sugar signals also affect the activities of FBA. There is growing interest in carbon-concentrating mechanisms (CCMs) in plants. Because FBA is an important enzyme involved in the Calvin cycle, improving the activity of the enzyme could certainly boost CO2 concentrations in plant green tissues.

In sum, the TaFBA gene family has significant biofunctions during plant development, metabolism, and abiotic stress responses. The TaFBA genes may be utilized in the development and selection of high-yield and multi-resistant wheat cultivars.

Author Contributions

Chromosomal location and express level experiment: GL and XG. Bioinformatics analysis and data processing: GL, LPX, and LX. Cultivating the wheat plants, sample collection, and mRNA extraction: YY and YT. Plant material, experiment design, discussion writing, and manuscripts review: CX, XZ, XP, AG, and HX.

Conflict of Interest Statement

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


The current work was supported by the National Natural Science Foundation of China (Grant Nos. 30971769 and 31371541). Special thanks to Prof. Chuang Ma for the manuscripts review and good suggestion. We thank LetPub ( for its linguistic assistance during the preparation of this manuscript.

Supplementary Material

The Supplementary Material for this article can be found online at:

Figure S1. Chromosomal location of TaFBA genes. (A) TaFBA1, 2, 3, 4, 7, 8, 11, 19, and 20 genes were mapped on different gene loci by wheat_2014_90K SNP gene chip. (B) TaFBA7, 8, 10, 12, 14, and 15 genes were mapped by Chinese_Spring_Deletion gene chip.

Figure S2. Pairwise alignments of FBA genes of wheat and wheat relatives. The picture was generated by MeV using hierarchical clustering method. The number above the dash line are the identity between cDNA sequences, and the number below the dash line represent the identity between gDNA sequences.

Figure S3. Transposable elements on TaFBA genomic DNA. Gene structures of FBAs analyzed by GSDS. Exons are shown as blue rectangles; introns are shown as thin lines. Untranslated regions (UTRs) are shown as double-sided wedges. Promoters are shown as light-blue rectangles. Long terminal repeat(LTRs) are shown as purple rectangles. Terminal inverted repeat (TIRs) are shown as red rectangles. Short interspersed nuclear element (SINEs) are shown as green rectangles. Other Transposable element (TEs) are shown as pink rectangles.

Figure S4. The alignment of FBA protein sequences among wheat and other species. (A) The activity sites among the TaFBA1~18 corresponded to those sites among FBA isozymes of rabbit and human. The activity sites are indicated in black frames. (B) The activity sites among TaFBA19~21 corresponded to those sites among FBA isozymes of Thermus aquaticus. The activity sites are indicated in black frames. The red stars represent substitution mutations and deletion sites.

Table S1. Pairwise alignments of TaFBA genes. The number above the dash line are the identity between cDNA sequences, and the number below the dash line represent the identity between amino acid sequences.

Table S2. Gene-specific primers for mapping and cloning.

Table S3. FBA genes of wheat and wheat relatives.

Table S4. Annotation of transposable elements on TaFBA genes.

Table S5. HMM search hits of FBA proteins.

Table S6. Annotation of cis-regulatory elements involved in phytohormone and abiotic stress response of plants.

Table S7. BLAST results of FBA genes from PLEXdb.

Table S8. Primers used for qRT–PCR.

DOC1. Promoter sequences of TaFBA genes.

TXT1. The TaFBA cDNA sequences.

TXT2. The TaFBA gDNA sequences.

TXT3. The TaFBA protein sequences.

TXT4. The FBA cDNA sequences of wheat relatives.

TXT5. The FBA gDNA sequences of wheat relatives.

TXT6. The FBA protein sequences of other species.


ADP-RF, ADP ribosylation factor; ALD, Aldolase; cFBA, cytosol fructose-1,6-bisphosphate aldolase; CpFBA, Chloroplast/plastid Fructose-1, 6-bisphosphate aldolase; DeoC, Deoxyribose-phosphate aldolase; DHAP, Dihydroxyacetone phosphate; DUF1357_C, Putative nucleotide-binding domain of sugar-metabolizing enzyme; DUF1537, Putative sugar-binding N-terminal domain; EDTA, Ethylene diamine tetraacetic acid; F_bP_aldolase, Fructose-bisphosphate aldolase class-II domain; FBA/FBPA, Fructose-1, 6-bisphosphate aldolase; FBP, Fructose-1, 6-bisphosphate; FBPase_3, Fructose-1, 6-bisphosphatase; GAP, Glyceraldehyde-3-phosphate; hiTAIL-PCR, high-efficient thermal asymmetric interlaced PCR; HXK, Hexokinase; LTR, Long terminal repeat; NAD, Nicotinamide adenine dinucleotide; NAD_binding_11, NAD-binding domain of NADP-dependent 3-hydroxyisobutyrate dehydrogenase; NAD_binding_2, NAD binding domain of 6-phosphogluconate dehydrogenase; NADP, Nicotinamide adenine dinucleotide phosphate; qRT-PCR, quantitative real-time PCR; SFBA, Sedoheptulose/Fructose-bisphosphate aldolase; SINE, Short interspersed nuclear element; SuBP, Sedoheptulose-1, 7-bisphosphate; TaFBA, Fructose-1, 6-bisphosphate aldolase of Triticum aestivum L.; TE, Transposable element; TIM, Triose-phosphate isomerase; TIR, Terminal inverted repeat.


Allen, A. E., Moustafa, A., Montsant, A., Eckert, A., Kroth, P. G., and Bowler, C. (2012). Evolution and functional diversification of fructose bisphosphate aldolase genes in photosynthetic marine diatoms. Mol. Biol. Evol. 29, 367–379. doi: 10.1093/molbev/msr223

PubMed Abstract | CrossRef Full Text | Google Scholar

Anderson, L. E., and Advani, V. R. (1970). Chloroplast and cytoplasmic enzymes: three distinct isoenzymes associated with the reductive pentose phosphate cycle. Plant Physiol. 45, 583–585. doi: 10.1104/pp.45.5.583

PubMed Abstract | CrossRef Full Text | Google Scholar

Anderson, L. E., Ringenberg, M. R., Brown, V. K., and Carol, A. A. (2005). Both chloroplastic and cytosolic phosphofructoaldolase isozymes are present in the pea leaf nucleus. Protoplasma 225, 235–242. doi: 10.1007/s00709-005-0099-1

PubMed Abstract | CrossRef Full Text | Google Scholar

Anderson, L. E., Wang, X., and Gibbons, J. T. (1995). Three enzymes of carbon metabolism or their antigenic analogs in pea leaf nuclei. Plant Physiol. 108, 659–667. doi: 10.1104/pp.108.2.659

PubMed Abstract | CrossRef Full Text | Google Scholar

Antia, N. J. (2007). Comparative studies on aldolase activity in marine planktonic algae, and their evolutionary significance. J. Phycol. 3, 81–85. doi: 10.1111/j.1529-8817.1967.tb04635.x

PubMed Abstract | CrossRef Full Text | Google Scholar

Berg, I. A., Kockelkorn, D., Ramos-Vera, W. H., Say, R. F., Zarzycki, J., Hügler, M., et al. (2010). Autotrophic carbon fixation in archaea. Nat. Rev. Microbiol. 8, 447–460. doi: 10.1038/nrmicro2365

PubMed Abstract | CrossRef Full Text | Google Scholar

Blom, N., and Sygusch, J. (1997). Product binding and role of the C-terminal region in Class I D-fructose 1, 6-bisphosphate aldolase. Nat. Struct. Biol. 4, 36–39. doi: 10.1038/nsb0197-36

PubMed Abstract | CrossRef Full Text | Google Scholar

Cai, B., Li, Q., Xu, Y., Yang, L., Bi, H., and Ai, X. (2016). Genome-wide analysis of the fructose 1,6-bisphosphate aldolase (FBA) gene family and functional characterization of FBA7 in tomato. Plant Physiol. Biochem. 108, 251–265. doi: 10.1016/j.plaphy.2016.07.019

PubMed Abstract | CrossRef Full Text | Google Scholar

Cho, Y. H., and Yoo, S. D. (2011). Signaling role of fructose mediated by FINS1/FBP in Arabidopsis thaliana. PLoS Genet. 7:e1001263. doi: 10.1371/journal.pgen.1001263

PubMed Abstract | CrossRef Full Text | Google Scholar

Choulet, F., Alberti, A., Theil, S., Glover, N., Barbe, V., Daron, J., et al. (2014). Structural and functional partitioning of bread wheat chromosome 3B. Science 345:1249721. doi: 10.1126/science.1249721

PubMed Abstract | CrossRef Full Text | Google Scholar

Cieśla, M., Mierzejewska, J., Adamczyk, M., Farrants, A. K., and Boguta, M. (2014). Fructose bisphosphate aldolase is involved in the control of RNA polymerase III-directed transcription. Biochim. Biophys. Acta 1843, 1103–1110. doi: 10.1016/j.bbamcr.2014.02.007

PubMed Abstract | CrossRef Full Text | Google Scholar

Civáň, P., Ivaničová, Z., and Brown, T. A. (2013). Reticulated origin of domesticated emmer wheat supports a dynamic model for the emergence of agriculture in the fertile crescent. PLoS ONE 8:e81955. doi: 10.1371/journal.pone.0081955

PubMed Abstract | CrossRef Full Text | Google Scholar

Dalby, A., Dauter, Z., and Littlechild, J. A. (1999). Crystal structure of human muscle aldolase complexed with fructose 1,6-bisphosphate: mechanistic implications. Protein Sci. 8, 291–297. doi: 10.1110/ps.8.2.291

PubMed Abstract | CrossRef Full Text | Google Scholar

Dash, S., Hemert, J. V., Hong, L., Wise, R. P., and Dickerson, J. A. (2012). PLEXdb: gene expression resources for plants and plant pathogens. Nucleic Acids Res. 40(Database issue):D1194. doi: 10.1093/nar/gkr938

PubMed Abstract | CrossRef Full Text | Google Scholar

Dennis, E. S., Gerlach, W. L., Walker, J. C., Lavin, M., and Peacock, W. J. (1988). Anaerobically regulated aldolase gene of maize. A chimaeric origin? J. Mol. Biol. 202, 759–767. doi: 10.1016/0022-2836(88)90556-6

PubMed Abstract | CrossRef Full Text | Google Scholar

Devos, K. M., Dubcovsky, J., Dvořák, J., Chinoy, C. N., and Gale, M. D. (1995). Structural evolution of wheat chromosomes 4a, 5a, and 7b and its impact on recombination. Theor. Appl. Genetics 91, 282–288. doi: 10.1007/BF00220890

PubMed Abstract | CrossRef Full Text | Google Scholar

Du, J., Say, R. F., Lü, W., Fuchs, G., and Einsle, O. (2011). Active-site remodelling in the bifunctional fructose-1,6-bisphosphate aldolase/phosphatase. Nature 478:534. doi: 10.1038/nature10458

PubMed Abstract | CrossRef Full Text | Google Scholar

Dubcovsky, J., and Dvorak, J. (2007). Genome plasticity a key factor in the success of polyploid wheat under domestication. Science 316, 1862–1866. doi: 10.1126/science.1143986

PubMed Abstract | CrossRef Full Text | Google Scholar

Dubcovsky, J., Luo, M.-C., and Dvorak, J. (1995). Differentiation between homoeologous chromosomes 1A of wheat and 1Am. of Triticum monococcum and its recognition by the wheat Ph1 locus. Proc. Natl Acad. Sci. U.S.A. 92, 6645–6649. doi: 10.1073/pnas.92.14.6645

PubMed Abstract | CrossRef Full Text | Google Scholar

Dvorak, J., McGuire, P. E., and Cassidy, B. (1988). Apparent sources of the A genomes of wheat inferred from polymorphism in abundance and restriction fragment of repeated nucleotide sequences. Genome 30, 680–689. doi: 10.1139/g88-115

CrossRef Full Text | Google Scholar

Escobar, J. S., Scornavacca, C., Cenci, A., Guilhaumon, C., Santoni, S., Douzery, E. J., et al. (2011). Multigenic phylogeny and analysis of tree incongruences in triticeae (poaceae). BMC Evol. Biol. 11:181. doi: 10.1186/1471-2148-11-181

PubMed Abstract | CrossRef Full Text | Google Scholar

Fan, W., Zhang, Z., and Zhang, Y. (2009). Cloning and molecular characterization of fructose-1,6-bisphosphate aldolase gene regulated by high-salinity and drought in Sesuvium portulacastrum. Plant Cell Rep. 28:975. doi: 10.1007/s00299-009-0702-6

PubMed Abstract | CrossRef Full Text | Google Scholar

Finn, R. D., Penelope, C., Eberhardt, R. Y., Eddy, S. R., Jaina, M., Mitchell, A. L., et al. (2016). The pfam protein families database: towards a more sustainable future. Nucleic Acids Res. 44(Database issue):D279–D285. doi: 10.1093/nar/gkv1344

PubMed Abstract | CrossRef Full Text | Google Scholar

Flechner, A., Gross, W., Martin, W. F., and Schnarrenberger, C. (1999). Chloroplast class I and class II aldolases are bifunctional for fructose-1,6-biphosphate and sedoheptulose-1,7-biphosphate cleavage in the Calvin cycle. FEBS Lett. 447, 200–202. doi: 10.1016/S0014-5793(99)00285-9

PubMed Abstract | CrossRef Full Text | Google Scholar

Gross, W., and Al, E. (1999). Characterization, cloning, and evolutionary history of the chloroplast and cytosolic class I aldolases of the red alga Galdieria sulphuraria. Gene 230, 7–14. doi: 10.1016/S0378-1119(99)00059-1

PubMed Abstract | CrossRef Full Text | Google Scholar

Gross, W., Bayer, M. G., Schnarrenberger, C., Gebhart, U. B., Maier, T. L., and Schenk, H. (1994). Two distinct aldolases of class II type in the cyanoplasts and in the cytosol of the alga Cyanophora paradoxa. Plant Physiol. 105, 1393–1398. doi: 10.1104/pp.105.4.1393

PubMed Abstract | CrossRef Full Text | Google Scholar

Henze, K., Morrison, H. G., Sogin, M. L., and Müller, M. (1998). Sequence and phylogenetic position of a class II aldolase gene in the amitochondriate protist, Giardia lamblia. Gene 222, 163–168. doi: 10.1016/S0378-1119(98)00499-5

PubMed Abstract | CrossRef Full Text | Google Scholar

Horton, P., Park, K. J., Obayashi, T., Fujita, N., Harada, H., Adams-Collier, C. J., et al. (2007). WoLF PSORT: protein localization predictor. Nucleic Acids Res. 35(Web Server issue), 585–587. doi: 10.1093/nar/gkm259

PubMed Abstract | CrossRef Full Text | Google Scholar

Hruz, T., Laule, O., Szabo, G., Wessendorp, F., Bleuler, S., Oertle, L., et al. (2008). Genevestigator V3: a reference expression database for the meta-analysis of transcriptomes. Adv. Bioinformatics 2008:420747. doi: 10.1155/2008/420747

PubMed Abstract | CrossRef Full Text | Google Scholar

Izard, T., and Sygusch, J. (2004). Induced fit movements and metal cofactor selectivity of class II aldolases: structure of Thermus aquaticus fructose-1,6-bisphosphate aldolase. J. Biol. Chem. 279, 11825–11833. doi: 10.1074/jbc.M311375200

PubMed Abstract | CrossRef Full Text | Google Scholar

Kagaya, Y., Nakamura, H., Hidaka, S., Ejiri, S., and Tsutsumi, K. (1995). The promoter from the rice nuclear gene encoding chloroplast aldolase confers mesophyll-specific and light-regulated expression in transgenic tobacco. Mol. Gen. Genet. 248, 668–674. doi: 10.1007/BF02191706

PubMed Abstract | CrossRef Full Text | Google Scholar

Khanna, S. M., Taxak, P. C., Jain, P. K., Saini, R., and Srinivasan, R. (2014). Glycolytic enzyme activities and gene expression in Cicer arietinum exposed to water-deficit stress. Appl. Biochem. Biotechnol. 173, 1–13. doi: 10.1007/s12010-014-1028-6

PubMed Abstract | CrossRef Full Text | Google Scholar

Krüger, I., and Schnarrenberger, C. (1983). Purification, subunit structure and immunological comparison of fructose-bisphosphate aldolases from spinach and corn leaves. Euro. J. Biochem. 136:101. doi: 10.1111/j.1432-1033.1983.tb07711.x

PubMed Abstract | CrossRef Full Text | Google Scholar

Labbé, G., Groot, S. D., Rasmusson, T., Milojevic, G., Dmitrienko, G. I., and Guillemette, J. G. (2011). Evaluation of four microbial Class II fructose 1,6-bisphosphate aldolase enzymes for use as biocatalysts. Protein Expr. Purif. 80, 224–233. doi: 10.1016/j.pep.2011.06.020

PubMed Abstract | CrossRef Full Text | Google Scholar

Lebherz, H. G., Leadbetter, M. M., and Bradshaw, R. A. (1984). Isolation and characterization of the cytosolic and chloroplast forms of spinach leaf fructose diphosphate aldolase. J. Biol. Chem. 259, 1011–1017.

PubMed Abstract | Google Scholar

Lebherz, H. G., and Rutter, W. J. (1969). Distribution of fructose diphosphate aldolase variants in biological systems. Biochemistry 8, 109–121. doi: 10.1021/bi00829a016

PubMed Abstract | CrossRef Full Text | Google Scholar

Li, L., Zhang, G. S., Zhang, L. Y., and Li, Y. X. (2012). Analysis of gene expression for manganese superoxide dismutase (Mn-SOD) and fructose-1.6-bisphosphate aldolase (FBA) in genetic and physiological male sterility lines of wheat. J. Agric. Biotechnol. 20, 225–234. doi: 10.3969/j.issn.1674-7968.2012.03.001

CrossRef Full Text | Google Scholar

Liu, Y. G., and Chen, Y. (2007). High-efficiency thermal asymmetric interlaced PCR for amplification of unknown flanking sequences. BioTechniques 43:649. doi: 10.2144/000112601

PubMed Abstract | CrossRef Full Text | Google Scholar

Lorentzen, E., Pohl, E., Zwart, P., Stark, A., Russell, R. B., Knura, T., et al. (2003). Crystal structure of an archaeal class I aldolase and the evolution of (ÃĆÂę α)8 barrel proteins. J. Biol. Chem. 278, 47253–47260. doi: 10.1074/jbc.M305922200

CrossRef Full Text | Google Scholar

Lorentzen, E., Siebers, B., Hensel, R., and Pohl, E. (2004). Structure, function and evolution of the Archaeal class I fructose-1,6-bisphosphate aldolase. Biochem. Soc. Trans. 32(Pt 2), 259–263. doi: 10.1042/bst0320259

PubMed Abstract | CrossRef Full Text | Google Scholar

Lu, W., Tang, X., Huo, Y., Xu, R., Qi, S., Huang, J., et al. (2012). Identification and characterization of fructose 1,6-bisphosphate aldolase genes in Arabidopsis reveal a gene family with diverse responses to abiotic stresses. Gene 503:65. doi: 10.1016/j.gene.2012.04.042

PubMed Abstract | CrossRef Full Text | Google Scholar

Marcussen, T., Sandve, S. R., Heier, L., Spannagl, M., Pfeifer, M., Jakobsen, K. S., et al. (2014). Ancient hybridizations among the ancestral genomes of bread wheat. Science 345:1250092. doi: 10.1126/science.1250092

PubMed Abstract | CrossRef Full Text | Google Scholar

Marsh, J. J., and Lebherz, H. G. (1992). Fructose-bisphosphate aldolases: an evolutionary history. Trends Biochem. Sci. 17, 110–113. doi: 10.1016/0968-0004(92)90247-7

PubMed Abstract | CrossRef Full Text | Google Scholar

Maurady, A., Zdanov, A., De, M. D., Beaudry, D., and Sygusch, J. (2002). A conserved glutamate residue exhibits multifunctional catalytic roles in D-fructose-1, 6-bisphosphate aldolases. J. Biol. Chem. 277, 9474–9483. doi: 10.1074/jbc.M107600200

PubMed Abstract | CrossRef Full Text | Google Scholar

Mayer, K. F. X., Rogers, J., Doležel, J., Pozniak, C., Eversole, K., Feuillet, C., et al. (2014). A chromsome-based draft sequence of the hexaploid bread wheat (Triticum aestivum) genome. Science 345:1251788. doi: 10.1126/science.1251788

CrossRef Full Text | Google Scholar

Michelis, R., and Gepstein, S. (2000). Identification and characterization of a heat-induced isoform of aldolase in oat chloroplast. Plant Mol. Biol. 44:487. doi: 10.1023/A:1026528319769

PubMed Abstract | CrossRef Full Text | Google Scholar

Mininno, M., Brugière, S., Pautre, V., Gilgen, A., Ma, S., et al. (2012). Characterization of chloroplastic fructose 1,6-bisphosphate aldolases as lysine-methylated proteins in plants. J. Biol. Chem. 287:21034. doi: 10.1074/jbc.M112.359976

PubMed Abstract | CrossRef Full Text | Google Scholar

Mohapatra, S., and Mittra, B. (2016). Protein glutathionylation protects wheat (Triticum aestivum Var. Sonalika) against Fusarium induced oxidative stress. Plant Physiol. Biochem. 109:319. doi: 10.1016/j.plaphy.2016.10.014

PubMed Abstract | CrossRef Full Text | Google Scholar

Oelze, M. L., Muthuramalingam, M., Vogel, M. O., and Dietz, K. J. (2014). The link between transcript regulation and de novo protein synthesis in the retrograde high light acclimation response of Arabidopsis thaliana. BMC Genomics 15:320. doi: 10.1186/1471-2164-15-320

PubMed Abstract | CrossRef Full Text | Google Scholar

Ohnishi, N., Himi, E., Yamasaki, Y., and Noda, K. (2008). Differential expression of three ABA-insensitive five binding protein (AFP)-like genes in wheat. Genes Genet. Syst. 83, 167–177. doi: 10.1266/ggs.83.167

PubMed Abstract | CrossRef Full Text | Google Scholar

Páez-Valencia, J., Valencia-Mayoral, P., Sánchez-Gómez, C., Contreras-Ramos, A., Hernández-Lucas, I., Martínez-Barajas, E., et al. (2008). Identification of Fructose-1, 6-bisphosphate aldolase cytosolic class I as an NMH7 MADS domain associated protein. Biochem. Biophys. Res. Commun. 376, 700–705. doi: 10.1016/j.bbrc.2008.09.064

PubMed Abstract | CrossRef Full Text | Google Scholar

Paolacci, A. R., Tanzarella, O. A., Porceddu, E., and Ciaffi, M. (2009). Identification and validation of reference genes for quantitative RT-PCR normalization in wheat. BMC Mol. Biol. 10:11. doi: 10.1186/1471-2199-10-11

PubMed Abstract | CrossRef Full Text | Google Scholar

Peltier, J. B., Cai, Y., Sun, Q., Zabrouskov, V., Giacomelli, L., Rudella, A., et al. (2006). The oligomeric stromal proteome of Arabidopsis thaliana chloroplasts. Mol. Cell. Proteomics 5, 114–133. doi: 10.1074/mcp.M500180-MCP200

PubMed Abstract | CrossRef Full Text | Google Scholar

Pelzer-Reith, B., Penger, A., and Schnarrenberger, C. (1993). Plant aldolase: cDNA and deduced amino-acid sequences of the chloroplast and cytosol enzyme from spinach. Plant Mol. Biol. 21, 331–340. doi: 10.1007/BF00019948

PubMed Abstract | CrossRef Full Text | Google Scholar

Penhoet, E., Kochman, M., Valentine, R., and Rutter, W. J. (1967). The subunit structure of mammalian fructose diphosphate aldolase. Biochemistry 6, 2940–2949. doi: 10.1021/bi00861a039

PubMed Abstract | CrossRef Full Text | Google Scholar

Perham, R. N. (1990). The fructose-1,6-bisphosphate aldolases: same reaction, different enzymes. Biochem. Soc. Trans. 18, 185–187. doi: 10.1042/bst0180185

PubMed Abstract | CrossRef Full Text | Google Scholar

Plaumann, M., Pelzer-Reith, B., Martin, W. F., and Schnarrenberger, C. (1997). Multiple recruitment of class-I aldolase to chloroplasts and eubacterial origin of eukaryotic class-II aldolases revealed by cDNAs from Euglena gracilis. Curr. Genet. 31, 430–438. doi: 10.1007/s002940050226

PubMed Abstract | CrossRef Full Text | Google Scholar

Purev, M., Kim, M. K., and Samdan, N. (2008). Isolation of a novel fructose- 1,6-bisphosphate aldolase gene from codonopsis lanceolata and analysis of the response of this gene to abiotic stresses. Mol. Biol. 42:179. doi: 10.1134/S0026893308020027

PubMed Abstract | CrossRef Full Text | Google Scholar

Rogers, M., and Keeling, P. J. (2004). Lateral transfer and recompartmentalization of Calvin cycle enzymes of plants and algae. J. Mol. Evol. 58, 367–375. doi: 10.1007/s00239-003-2558-7

PubMed Abstract | CrossRef Full Text | Google Scholar

Rolland, F., Baenagonzalez, E., and Sheen, J. (2006). Sugar sensing and signaling in plants: conserved and novel mechanisms. Annu. Rev. Plant Biol. 57, 675–709. doi: 10.1146/annurev.arplant.57.032905.105441

PubMed Abstract | CrossRef Full Text | Google Scholar

Ronimus, R. S., and Morgan, H. W. (2003). Distribution and phylogenies of enzymes of the embden-meyerhof-parnas pathway from archaea and hyperthermophilic bacteria support a gluconeogenic origin of metabolism. Archaea 1:199. doi: 10.1155/2003/162593

PubMed Abstract | CrossRef Full Text | Google Scholar

Rutter, W. J. (1964). Evolution of aldolase. Fed. Proc. 23, 1248–1257.

PubMed Abstract | Google Scholar

Sánchez, L. B., Horner, D. S., Moore, D. V., Henze, K., Embley, T. M., and Müller, M. (2002). Fructose-1,6-bisphosphate aldolases in amitochondriate protists constitute a single protein subfamily with eubacterial relationships. Gene 295, 51–59. doi: 10.1016/S0378-1119(02)00804-1

PubMed Abstract | CrossRef Full Text | Google Scholar

Sarry, J. E., Kuhn, L., Ducruix, C., Lafaye, A., Junot, C., Hugouvieux, V., et al. (2006). The early responses of Arabidopsis thaliana cells to cadmium exposure explored by protein and metabolite profiling analyses. Proteomics 6, 2180–2198. doi: 10.1002/pmic.200500543

PubMed Abstract | CrossRef Full Text | Google Scholar

Sauvé, V., and Sygusch, J. (2001). Molecular cloning, expression, purification, and characterization of fructose-1,6-bisphosphate aldolase from Thermus aquaticus. Protein Expr. Purif. 21:293. doi: 10.1006/prep.2000.1380

PubMed Abstract | CrossRef Full Text | Google Scholar

Schnarrenberger, C., and Krüger, I. (1986). Distinction between cytosol and chloroplast fructose-bisphosphate aldolases from pea, wheat, and corn leaves. Plant Physiol. 80, 301–304. doi: 10.1104/pp.80.2.301

PubMed Abstract | CrossRef Full Text | Google Scholar

Schwede, T., Kopp, J., Guex, N., and Peitsch, M. C. (2003). SWISS-MODEL: an automated protein homology-modeling server. Nucleic Acids Res. 31, 3381–3385. doi: 10.1093/nar/gkg520

PubMed Abstract | CrossRef Full Text | Google Scholar

Sears, E. R., Riley, R., and Lewis, K. R. (1966). “Nullisomictetrasomic combinations in hexaploid wheat,” in Chromosome Manipulations and Plant Genetics, eds R. Riley and K. R. Lewis (London: Oliver and Boyd), 29–45.

Sherawat, M., Tolan, D. R., and Allen, K. N. (2008). Structure of a rabbit muscle fructose-1,6-bisphosphate aldolase A dimer variant. Acta Crystallogr. D Biol. Crystallogr. 64, 543–550. doi: 10.1107/S0907444908004976

PubMed Abstract | CrossRef Full Text | Google Scholar

Sievers, F., Wilm, A., Dineen, D., Gibson, T. J., Karplus, K., Li, W., et al. (2011). Fast, scalable generation of high-quality protein multiple sequence alignments using Clustal Omega. Mol. Syst. Biol. 7, 1429–1432. doi: 10.1038/msb.2011.75

PubMed Abstract | CrossRef Full Text

Tamura, K., Peterson, D., Peterson, N., Stecher, G., Nei, M., and Kumar, S. (2011). MEGA5: molecular evolutionary genetics analysis using maximum likelihood, evolutionary distance, and maximum parsimony methods. Mol. Biol. Evol. 28, 2731–2739. doi: 10.1093/molbev/msr121

PubMed Abstract | CrossRef Full Text | Google Scholar

Tolan, D. R., Niclas, J., Bruce, B. D., and Lebo, R. V. (1987). Evolutionary implications of the human aldolase-A, -B, -C, and -pseudogene chromosome locations. Am. J. Hum. Genet. 41, 907–924.

PubMed Abstract | Google Scholar

Willard, J. M., and Gibbs, M. (1968). Role of Aldolase in Photosynthesis. II Demonstration of aldolase types in photosynthetic organisms. Plant Physiol. 43, 793–798. doi: 10.1104/pp.43.5.793

PubMed Abstract | CrossRef Full Text | Google Scholar

Xu, G., Guo, C., Shan, H., and Kong, H. (2012). Divergence of duplicate genes in exon-intron structure. Proc. Natl. Acad. Sci. U.S.A. 109, 1187–1192. doi: 10.1073/pnas.1109047109

PubMed Abstract | CrossRef Full Text | Google Scholar

Xue, G. P., Mcintyre, C. L., Glassop, D., and Shorter, R. (2008). Use of expression analysis to dissect alterations in carbohydrate metabolism in wheat leaves during drought stress. Plant Mol. Biol. 67, 197–214. doi: 10.1007/s11103-008-9311-y

PubMed Abstract | CrossRef Full Text | Google Scholar

Yamada, S., Komori, T., Hashimoto, A., Kuwata, S., Imaseki, H., and Kubo, T. (2000). Differential expression of plastidic aldolase genes in Nicotiana plants under salt stress. Plant Sci. 154, 61–69. doi: 10.1016/s0168-9452(00)00188-6

PubMed Abstract | CrossRef Full Text | Google Scholar

Zeng, L., Deng, R., Guo, Z., Yang, S., and Deng, X. (2016). Genome-wide identification and characterization of glyceraldehyde-3-phosphate dehydrogenase genes family in wheat (Triticum aestivum). BMC Genomics 17:240. doi: 10.1186/s12864-016-2527-3

PubMed Abstract | CrossRef Full Text | Google Scholar

Zeng, Y., Tan, X., Zhang, L., Jiang, N., and Cao, H. (2014). Identification and expression of fructose-1,6-bisphosphate aldolase genes and their relations to oil content in developing seeds of tea oil tree (Camellia oleifera). PLoS ONE 9:e107422. doi: 10.1371/journal.pone.0107422

PubMed Abstract | CrossRef Full Text | Google Scholar

Zhang, G., Liu, Y., Ni, Y., Meng, Z., Lu, T., and Li, T. (2014). Exogenous calcium alleviates low night temperature stress on the photosynthetic apparatus of tomato leaves. PLoS ONE 9:e97322. doi: 10.1371/journal.pone.0097322

PubMed Abstract | CrossRef Full Text | Google Scholar

Zhang, Y. (2008). I-TASSER server for protein 3D structure prediction. BMC Bioinformatics 9:40. doi: 10.1186/1471-2105-9-40

PubMed Abstract | CrossRef Full Text | Google Scholar

Zhang, Z., and Wood, W. I. (2003). A profile hidden Markov model for signal peptides generated by HMMER. Bioinformatics 19, 307–308. doi: 10.1093/bioinformatics/19.2.307

PubMed Abstract | CrossRef Full Text | Google Scholar

Zhao, Y., Cai, M., Zhang, X., Li, Y., Zhang, J., Zhao, H., et al. (2014). Genome-wide identification, evolution and expression analysis of mterf gene family in maize. PLoS ONE 9:e94126. doi: 10.1371/journal.pone.0094126

PubMed Abstract | CrossRef Full Text | Google Scholar

Keywords: FBA, wheat, chromosomal localization, genomic structure, protein structure, expression analysis, light/dark treatment, abiotic stress responses

Citation: Lv G-Y, Guo X-G, Xie L-P, Xie C-G, Zhang X-H, Yang Y, Xiao L, Tang Y-Y, Pan X-L, Guo A-G and Xu H (2017) Molecular Characterization, Gene Evolution, and Expression Analysis of the Fructose-1, 6-bisphosphate Aldolase (FBA) Gene Family in Wheat (Triticum aestivum L.). Front. Plant Sci. 8:1030. doi: 10.3389/fpls.2017.01030

Received: 28 February 2017; Accepted: 29 May 2017;
Published: 14 June 2017.

Edited by:

Petr Smýkal, Palacký University, Olomouc, Czechia

Reviewed by:

Jan Šafář, Institute of Experimental Botany (ASCR), Czechia
Tomáš Vyhnánek, Mendel University, Czechia
Dariusz Grzebelus, University of Agriculture in Krakow, Poland

Copyright © 2017 Lv, Guo, Xie, Xie, Zhang, Yang, Xiao, Tang, Pan, Guo and Xu. This is an open-access article distributed under the terms of the Creative Commons Attribution License (CC BY). The use, distribution or reproduction in other forums is permitted, provided the original author(s) or licensor are credited and that the original publication in this journal is cited, in accordance with accepted academic practice. No use, distribution or reproduction is permitted which does not comply with these terms.

*Correspondence: Hong Xu,