Original Research ARTICLE
Genome-Wide Characterization and Expression Profiling of Sugar Transporter Family in the Whitefly, Bemisia tabaci (Gennadius) (Hemiptera: Aleyrodidae)
- 1College of Plant Protection, Hunan Agricultural University, Changsha, China
- 2Department of Plant Protection, Institute of Vegetables and Flowers, Chinese Academy of Agricultural Sciences, Beijing, China
- 3Department of Biocontrol, Institute of Plant Protection, Heilongjiang Academy of Agricultural Sciences, Harbin, China
- 4Key Laboratory of Bio-Pesticide Innovation and Application of Guangdong Province, Department of Entomology, South China Agricultural University, Guangzhou, China
- 5Key Laboratory of Molecular Biology of Heilongjiang Province, College of Life Sciences, Heilongjiang University, Harbin, China
Sugar transporters (STs) play pivotal roles in the growth, development, and stress responses of phloem-sucking insects, such as the whitefly, Bemisia tabaci. In this study, 137 sugar transporters (STs) were identified based on analysis of the genome and transcriptome of B. tabaci MEAM1. B. tabaci MEAM1 encodes a larger number of STs than other selected insects. Phylogenetic and molecular evolution analysis showed that the 137 STs formed three expanded clades and that the genes in Sternorrhyncha expanded clades had accelerated rates of evolution. B. tabaci sugar transporters (BTSTs) were divided into three groups based on their expression profiles across developmental stages; however, no host-specific BTST was found in B. tabaci fed on different host plants. Feeding of B. tabaci adults with feeding diet containing dsRNA significantly reduced the transcript level of the target genes in B. tabaci and mortality was significantly improved in B. tabaci fed on dsRNA compared to the control, which indicates the sugar transporters may be used as potential RNAi targets for B. tabaci bio-control. These results provide a foundation for further studies of STs in B. tabaci.
In multicellular organisms, sugars provide energy and carbon skeletons but are also involved in signaling and osmotic processes. Sugar, however, cannot directly pass through the cell membrane and the exchange of sugars between cells or between subcellular structures is mediated by sugar transporters (STs). Sugar transporters belong to the major facilitator superfamily (MFS). The MFS contains at least 24 distinct families with more than 249,360 sequenced members and shares a conserved 12 transmembrane domains, which is organized into two pseudosymmetrical halves (Yan, 2015). Because they are involved in sugar transport, STs are often the focus of MFS studies. In humans, STs are related to diabetes and have therapeutic importance because they mediate sugar movement across cancer cells (Wright et al., 2007). In plants, STs are critical for crop yield and are involved in resistance against pathogens (Doidy et al., 2012; Schroeder et al., 2013).
The whitefly Bemisia tabaci (Gennadius) is a globally distributed polyphagous pest that includes a number of genetically divergent but morphologically indistinguishable species (De Barro et al., 2011; Liu et al., 2012; Boykin and De Barro, 2014). Two of these species, MEAM1 (formerly cryptic species “B”) and MED (formerly cryptic species “Q”), are major agricultural pests in more than 60 countries (Chu et al., 2006; De Barro et al., 2011; Pan et al., 2011, 2015). B. tabaci damages plants both directly by sucking phloem sap and indirectly by transmitting plant viruses (Jones, 2003; De Barro et al., 2011; Pan et al., 2012a). As a diet, phloem sap contains low levels of nitrogen and essential amino acids. In the pea aphid, Acyrthosiphon pisum, for example, two STs were reported to be up-regulated in the bacterocyte (Hansen and Moran, 2011). The bacterial symbionts in phloem-feeding insects provide the essential amino acids and vitamins that compensate for the lack of essential amino acids in phloem sap (Baumann, 2005; Pan et al., 2012b). Sugar transporters are very important for B. tabaci. First, B. tabaci ingests only plant sap, which contains sucrose (Byrne and Miller, 1990; Hayashi and Chino, 1990), the ingested sucrose, however, cannot directly pass across the gut epithelium and is hydrolyzed into glucose and fructose in the gut. Transport of glucose and fructose across the gut epithelium is mediated by STs (Ashford et al., 2000; Cristofoletti et al., 2003; Price et al., 2007a). In addition, trehalose, the principal sugar circulating in the blood or haemolymph of most insects (Thompson, 2003), is also transported by STs (Kikawada et al., 2007). Thus, STs are essential for sugar exchange in B. tabaci. Second, although the concentration and osmotic pressure of phloem sap varies among plants, the osmotic pressure is always higher in phloem sap than in the phloem-feeding insect (Douglas, 2006). To prevent loss of water in response to this difference in osmotic pressure, phloem-feeding insects have developed an osmoregulation mechanism. Sugar transporters contribute to osmoregulation by importing sugars, mainly glucose, from the gut lumen into cells (Price et al., 2007b; Kikuta et al., 2015; Tzin et al., 2015). Third, the interactions between B. tabaci and virus may require STs. Sugar transporters are receptors for human T cell leukemia virus and white spot syndrome virus (Manel et al., 2003; Huang et al., 2012). A recent study found that an ST was up-regulated in Bombyx mori infected with B. mori nucleopolyhedrovirus and that the expression levels of three STs differed in virus-susceptible vs. -resistant strains (Sagisaka et al., 2010; Govindaraj et al., 2016). Although five genera of plant viruses are transmitted by B. tabaci (Jones, 2003), the interactions between B. tabaci and viruses are unclear at the molecular level but might involve STs.
Several recent studies have reported on STs from insects (Kikawada et al., 2007; Liu et al., 2013; Govindaraj et al., 2016), including phloem-feeding insects (Price et al., 2007b, 2010; Kikuta et al., 2010; Price and Gatehouse, 2014; Ge et al., 2015). For example, genomic studies identified STs in the pea aphid, A. pisum (Price et al., 2010; Price and Gatehouse, 2014). Among those STs, APST3, and APST4 were determined to be highly expressed in the gut (Price et al., 2010; Price and Gatehouse, 2014). Functional analysis showed that APST3 and APST4 were a low affinity transporter and a high affinity transporter of glucose and fructose, respectively (Price et al., 2010; Price and Gatehouse, 2014). In another study, 18 putative STs were identified in the brown planthopper, Nilaparvata lugens, and seven of them were highly expressed in the gut (Kikuta et al., 2010). Further analysis revealed that NlST1 and NlST16 were glucose transporters and that NIST6 was a fructose transporter (Price et al., 2007b; Kikuta et al., 2010, 2015).
In the current study, a genome-wide approach was used to investigate the STs in B. tabaci. Our overall goal was to increase our understanding of these STs and to identify STs that might serve as targets for controlling B. tabaci. We first identified STs in B. tabaci MEAM1 (hereafter BTSTs) based on its genome and transcriptomic datasets. In addition, STs from the following 11 other insect species were identified based on their genomes: A. pisum, Diaphorina citri, Nasonia vitripennis, Apis mellifera, Musca domestica, Drosophila melanogaster, Anopheles gambiae, Aedes aegypti, Manduca sexta, Plutella xylostella, and B. mori. Next, the phylogenetic relationships were analyzed among BTSTs and the STs from seven other insect species, and evolutional pattern of expanded BTSTs were investigated. The gene expression patterns of BTSTs were then measured based on the transcriptome datasets, which included B. tabaci samples from different developmental stages and different host plants. Reverse transcriptase-quantitative polymerase chain reaction (RT-qPCR) was used to verify the BTSTs expression patterns across different stages. Finally, we determined the effect of orally delivered dsRNAs of nine BTSTs on the motality of B. tabaci MEAM1.
Materials and Methods
De novo Identification of STs in B. tabaci and Other Insects
The version of the genome of China B. tabaci MEAM1 (http://184.108.40.206/download/) were annotated by homolog search and de novo predicting and transcriptome/EST correspondence. To search for all STs in the reference protein dataset, predicted proteins that matched the Pfam HMM (Hidden Markov model) profile of sugar transporter (PF00083) were identified by hmmsearch (HMMER software, version 3.1b1) with an E-value <0.001 (Eddy, 2011; Finn et al., 2016), and the identified STs were used as query to search the B. tabaci MEAM1 genome again to avoid missing annotation. Next, the identified 228 putative proteins were annotated by blasting against the NR database (Version 2015.6) with the blastp program (Altschul et al., 1997). Proteins that did not match known STs with an E-value <0.001 were excluded. After that, the identified STs were searched against B. tabaci transcripts database (Xie et al., 2014; SRP064690) [de novo assembled using the transcriptome sequencing data by Trinity software (Haas et al., 2013)] using the tblastn program (Altschul et al., 1997). Then, manual corrections were preformed. Finally, whether the corrected STs contained TIGR00879 with a score above 237.80 and an E-value <0.001 was determined using hmmsearch (HMMER software version 3.1b1) (Haft et al., 2001; Eddy, 2011). Trans-membrane regions were predicted using the TOPCONS Server (http://topcons.cbr.su.se/) (Bernsel et al., 2009).
To compare the composition and diversity of BTSTs with STs from other insects, STs were identified in the reference protein datasets of 11 other insect species using the pipelines described above. The information of the selected datasets is provided in Table S1.
Insect Strain and RNAseq Samples Preparation, RNA Isolation, cDNA Library Construction, and Illumina Sequencing
The strain of B. tabaci MEAM1 BtB1-China population was originally collected in 2004 from cabbage, Brassica oleracea cv. Jingfeng1, in Beijing and was subsequently reared on cotton in separate screen cages in a glasshouse. The purity of the culture was monitored every 2–3 generations based on haplotypes of the DNA sequence obtained using mtCOI primers (Chu et al., 2010).
For The different developmental stage samples (eggs, L1–L2, L3, L4 nymph, females, and males) were collected from BtB1-China population. Since distinguishing first and second nymph is laborious, a mixture of first and second nymphs was collected as one sample. Only 2-h-old adults were collected using a glass tube (5 × 0.5 cm), the sex was determined under a stereo microscope and same sex female or males pooled into a plastic tube using an aspirator. Total RNA was extracted using Trizol reagent (Invitrogen) according to the manufacturer's instructions, and purity and degradation were checked on 1% agarose gels. RNA-seq libraries were constructed as previously described (Xie et al., 2014) and sequenced on a HiSeq 2500 system according to the manufacturer's instructions with sequenced at 125 bp (PE125, library size is 280–320 bp).
Genome-Wide Expression Analysis of BTSTs
The expression patterns of BTSTs were investigated by using a series of different developmental stage transcriptome sequencing data (SRP064690) as described above and B. tabaci from different host plants (Xie et al., 2014). Initially, all of the transcriptome datasets were filtered with Trimmomatic with default parameters (Bolger et al., 2014). The clean data were then mapped to the B. tabaci MEAM1 genome by TopHat v2.1.0 (Trapnell et al., 2009). Transcript expression, represented as FPKM, was calculated using Cufflinks v2.2.1 without taking splicing isoforms into account (Trapnell et al., 2012). Finally, The FPKM values were log transformed, and genes were clustered in term of expression patterm by Cluster 3.0 and visualized by Treeview software (Saldanha, 2004).
Phylogenetic Analysis of STs
To understand the phylogenetic relationship of BTSTs with STs from other insects, amino acid sequences of BTSTs and STs of seven other insect species were used to conduct phylogenetic analysis. To perform a high quality phylogenetic analysis, full-length sequences that contained > 250 amino acid residues were aligned by MAFFT software v7.221 with the L-ins-I method (Katoh et al., 2002). The alignment was trimmed in Trimal using a gap throughout of 25% (Capella-Gutierrez et al., 2009). The phylogenetic tree was estimated using a maximum-likelihood (ML) method. Before the phylogenetic analysis was performed, the best-fit model LG+I+G+F was determined by Prottest 3.4 (Abascal et al., 2005). ML analysis was then conducted by Raxml V8.2.4 with 1,000 replicates using the fast bootstrap option (Stamatakis, 2014). Finally, the result was visualized by iTOL (Letunic and Bork, 2007).
Positive Selection and ST Gene Conservation Analysis
To further understand the BTSTs expanded clades, molecular evolutional rates of those STs were estimated. Before the molecular evolutionary analysis, the amino acid sequences of the expanded STs were aligned by MAFFT, and their phylogeny tree was constructed by Mrbayse V3.2 (Huelsenbeck and Ronquist, 2001). Because the LG protein substitution matrix is not available in Mrbayse, the phylogeny was constructed using WAG+F+I+G. Finally, the tree was used as the input file for further molecular evolution analysis.
In our study, the branch-based models and site-based models of molecular evolution were selected and analyzed by Paml 4.9a software (Yang, 2007). Non-synonymous/synonymous substitution rate ratios (dN/dS) of all selected STs were estimated based on their coding sequence (CDS). A dN/dS ratio >1 indicates positive selection, a dN/dS ratio <1 indicates purifying selection, and a dN/dS ratio = 1 indicates neutral evolution. Both branch-based models and site-based models were tested as described previously (Price et al., 2011). In brief, for branch models of molecular evolution, a series of ω categories were calculated (model = 0 or 2, NS sites = 0). The other parameters, ω and κ, started from 0.2 to 2, respectively, and the coding frequency was using 3 * 4 codon table. The bayesian trees of BTST expanded clades with assigned ω were shown in Figure S1 and the models of molecular evolutional test were shown in Table S2. For sie-based models of molecular evolution, three pairs of models were used: M0/M3, M1a/M2a, and M7/M8.
RNA Extraction and cDNA Synthesis
Total RNA was extracted from different stages of B. tabaci using TRIzol reagent following the manufacturer's recommendation (Invitrogen, Carlsbad, CA, USA). Gel electrophoresis and a NanoDrop 2000 c spectrophotometer (Thermo Fisher Scientific Inc., Waltham, MA, USA) was used to determine the quantity of RNA. PrimeScript™ II 1st strand cDNA Synthesis Kit (TaKaRa, Dalian, China) and PrimeScript RT kit (containing gDNA Eraser, Perfect Real Time, TaKaRa, Dalian, China) were used for preparing first-strand cDNA for cloning and gene expression analysis, respectively. The first-strand cDNA was stored at −20°C until used.
Cloning of BTSTs
Primers of selected BTSTs (Table S3) were designed based on their complete coding sequences. PCR reactions were performed in an S1000 TM Thermal Cycler PCR system with the following parameters: initial denaturation at 94°C for 10 min; followed by 35 cycles of denaturation at 94°C for 60 s, annealing at 55–60°C for 45 s, and extension at 72°C for 120 s; and a final extension at 72°C for 10 min using La-Taq polymerase (TaKaRa, Dalian, China). For BTST40 and BTST107, the PCR reaction system (25 μl volume in total) contained 2 μl of cDNA template, 2.5 μl of 10 × PCR buffer (Mg2+), 4 μl of dNTP mixture (2.5 mM), 0.25 μl of La-Taq, 1 μl of each primer (10 mM), and 14.25 μl of ddH2O. For the seven other BTSTs, the PCR reaction system (25 μl total volume) contained 2 μl of cDNA template, 12.5 μl of 2 × GC I buffer (Mg2+), 2 μl of dNTP mixture (2.5 mM), 0.25 μl of La-Taq, 1 μl of each primer (10 mM), and 6.25 μl of ddH2O. Amplicons of the expected bands were excised from 1.5% agarose gel, purified using the TIANgel Midi Purification Kit (TIANGEN, Beijing, China), and subcloned into the pEASY-T1 vector (Transgen, Beijing, China) before transformation into Escherichia coli TOP10 competent cells (Transgen, Beijing, China) for sequencing.
The RT-qPCR (ABI 7500 Real-Time PCR system, Applied Biosystems, USA) was used and specific primers (Table S4) were designed to investigate the expression levels of 15 BTSTs. The reaction mixture (25 μl) contained 9.5 μl of ddH2O, 12.5 μl of 2 × SuperReal PreMix Plus (TIANGEN, Beijing, China), 7.5 μM of both upstream and downstream primers, 1 μl of first-strand cDNA template, and 0.5 μl of 50 × ROX Reference Dye (TIANGEN, Beijing, China) based on the manufacturer's recommendations. The RT-qPCR program had the following parameters: initial denaturation for 15 min at 95°C followed by 40 cycles of denaturation at 95°C for 15 s, annealing for 30 s at 59–60°C, and extension for 32 s at 72°C. Finally, an automatic dissociation step for melting curve analysis was used. The standard curve for each candidate gene was generated from cDNA 2-fold serial dilutions (1/1, 1/2, 1/4, 1/8, and 1/16). The corresponding RT-qPCR efficiencies (E) are expressed as percentages according to the equation: E = (10[−1/slope] –1) × 100. Primer sets that showed a single peak in melting curve analyses, 90–110% primer amplification efficiencies, and > 0.95 coefficients (R2 values) were used for subsequent experiments. Conventional PCRs were performed before RT-qPCRs. The amplified fragments were sequenced to confirm. Four technical replicates and three biological replicates were used for each treatment. For negative control reactions, ddH2O was used in place of the cDNA template. Data were normalized to the elongation factor 1 alpha gene (Li et al., 2013), and relative gene expression was calculated using the 2−ΔΔCt method (Livak and Schmittgen, 2001).
Based on the genomic and transcriptome data, unique regions of selected STs were used as templates for dsRNA synthesis. The dsRNA for enhanced green fluorescent protein (EGFP) was used as the negative control. Primers are listed in Table S5. DsRNAs were prepared according to the T7 RiboMAX Express RNAi system protocols (Promega, Madison, USA). The RNAi bioassay was performed by directly feeding dsRNA to B. tabaci adults in a feeding chamber for 4 days. A 0.20-ml drop of diet solution that combined 5% yeast extract and 30% sucrose (wt/vol) with 100 ng of dsRNA was placed in the chamber. The details of feeding were performed as described in previous studies (Yang et al., 2016). Approximately 50 adults (2 days old, mixed sexes) were used for each ST gene treatment, and each treatment was represented by three biological replicates. The experiment was conducted in an environmental chamber at 25°C, a photoperiod of L14: D10, and 80% RH. After 2 and 4 days, mortality was recorded and B. tabaci specimens were collected for analysis of the expression levels of targeted ST genes.
One-way ANOVA was used to compare the gene expression levels and mortality rates among different treatments. Means were compared with LSD tests at P < 0.05. SPSS version 20.0 (SPSS Inc., Chicago, IL, USA) was used for statistical analyses.
Identification of BTSTs
To obtain a genome-wide identification of BTSTs, we searched the predicting protein sequences of B. tabaci for the PF00083 (Sugar and other transporter). This resulted in the identification of coding sequences. Blasting against non-redundant protein 176 sequence (Nr) database subsequently showed that these coding sequences could be divided into three sub-families: STs, organic cation transporters, and synaptic vesicle proteins. Coding sequences that matched STs were then selected and manually corrected. Finally, 137 BTSTs were identified (Tables S7–S9). Among them, nine proteins matched the sugar transporter family motif TIGR000879 with scores above the cutoff. Sequence analyses revealed that most of the BTSTs contained the 12 transmembrane and that all of the BTSTs genes contained multiple exons except the gene coding BTST65, which was intron-less. In addition, some BTSTs formed different gene clusters that were located on different scaffold; for example, BTST10 to BTST17, BTST29 to BTST35, BTST53 to BTST57, and BTST112 to BTST119 were located on scaffold 15, 44, 149, and 1368, respectively (Figure 1). The tandem repeated pattern can be accounted for the expansion of BTSTs. Based on B. tabaci transcriptome datasets that were derived from different developmental stages and different host plants, 134 coding sequences had transcriptome coverage, suggesting that they were expressed in B. tabaci.
Figure 1. Location of tandem repeat BTSTs on scaffolds. The blue arrows indicate the transcriptional orientations of the BTSTs on the scaffolds. One BTST cluster was identified on each of four scaffolds (15, 44, 149, and 1,368).
Expression Profiles of BTSTs
The expression patterns of BTSTs were investigated using RNA-seq datasets obtained from different developmental stages of B. tabaci. The egg stage clustered separately from the other stages, whereas the 3rd and the 4th instars clustered together with female and male adults (Figure 2, Table S10). Transcript expression of most BTSTs was the lowest in eggs and the highest in adults, and only a few BTSTs exhibited a stage-specific expression pattern. Based on the expression values, the BTSTs could be divided into three groups. Group 1 contained 41 BTSTs, which were expressed in all developmental stages; among these, 15 BTSTs were highly expressed. Group 2 contained 33 BTSTs, which had low levels of expression and in some cases were not expressed in one or two stages. Most BTSTs in group 2 were not expressed in eggs, while the expression of BTST40, BTST44, BTST80, and BTST5 was low in eggs but was high in other stages. Group 3 contained 63 BTSTs, which were expressed in fewer than three stages, i.e., group 3 contained stage-specific BTSTs. For example, a male-specific gene BTST33 and a female-specific gene BTST76 were identified, although they were weakly expressed; the expression level of BTST124 was higher in adults than in eggs (fold-change: female vs. egg = 41, male vs. egg = 36); and expression levels of BTST1 and BTST68 were the highest in eggs and nymphs (1st and 2nd), respectively. To test and verify the RNA-seq-based expression results, expression patterns of 15 BTSTs across different stages were measured by RT-qPCR, and the results were consistent with the RNA-seq results (Figure 3).
Figure 2. Gene expression of BTSTs across different developmental stages. The log2(FPKM) values are presented as a heatmap. Bright yellow indicates higher expression values, dark blue indicates lower expression values, and gray indicates missing values. E, eggs; N1-2, 1st and 2nd instar nymphs; N3, 3rd instar nymphs; N4, 4th instar nymphs; M, males; F, females. (A) Group 1; (B) Group 2; (C) Group 3.
Figure 3. Expression profiling of BTSTs across different developmental stages based on RT-qPCR. E, eggs; N1-2, 1st and 2nd instar nymphs; N3, 3rd instar nymphs; N4, 4th instar nymphs; A, female and male adults.
RNA-seq data were also used to investigate how the expression profiles of BTSTs were affected by host plants. The results showed that expression was more affected by B. tabaci sex rather than by host plants (Figure 4, Table S11). Although the expression patterns of all BTSTs were not the same on all hosts, no host-specific BTST was identified.
Figure 4. Gene expression of BTSTs in male and female adults that fed on different host plants. CaF, females reared on cabbage; CaM, males reared on cabbage; CuF, females reared on cucumber; CuM, males reared on cucumber; CoF, females reared on cotton; CoM, males reared on cotton. ToF, females reared on tomato; ToM, males reared on tomato. (A) Group 1; (B) Group 2; (C) Group 3.
Phylogenetic Analysis of STs
Sugar transporters from the other 11 insect species were also identified. The number of STs varied among these insects (Table 1). Insects in the Hymenoptera and Diptera encoded fewer STs than insects in the Sternorrhyncha and Lepidoptera. The number of STs was greater in B. tabaci than in the other 11 insects (Table 1). Phylogenetic analysis showed that STs from the 12 insects formed several conspicuous, expanded clades (Figure 5). In addition to shared expanded clades that included insects from multiple orders, there were two Sternorrhyncha, two Lepidoptera, and one Diptera expanded clades. Number of STs in each of the expanded clades in the Lepidoptera and Sternorrhyncha expanded clades was more than it in the Diptera expanded clade. Interestingly, B. tabaci contributed more STs to the Sternorrhyncha expanded clades than A. pisum.
Figure 5. A maximum-likelihood tree of STs in B. tabaci and seven other insects. The analysis was constructed with Raxml V8.2.4 and the LG+F+I+G model. Bootstrap values expressed as percentages of 1000 replications are shown at branch points. Sternorrhyncha (AP, A. pisum, orange; BT, B. tabaci, red), Hymenoptera (AM, A. mellifera, blue; NV, N. vitripennis, brown), Diptera (AA, A. aegypti, cyan; DM, D. melanogaster, green), Lepidoptera (BM, B. mori, dark purple; MS, M. sexta, bright purple).
Molecular Evolution Analysis of STs
As indicated in the previous section, phylogenetic analysis showed that STs from the selected insect species formed several expanded clades. Several tandem repeat genes were also identified in the expanded clades. To test whether the BTSTs in Sternorrhyncha expanded clades have accelerated rates of evolution, a series of molecular evolution tests were performed. For all BTSTs in the two Sternorrhyncha expanded clades, the significantly improved likelihood estimated for the two ratios model compared with one ratio model suggested the BTSTs of the expanded clades evolved, on the average, at a higher rate than the STs outside the expanded clades (Table 2). We then tested the hypothesis that the evolutionary rates of BTSTs in expanded clades were consistent with their expression levels. Differences in lnL values were not significant when two ratios model was compared with three-ratio model. However, lnL values were significantly different when the more ratios model was compared with the two ratios model. The results indicated that BTSTs had different evolution rates within expanded clades.
Table 2. Results of the B. tabaci Sternorrhyncha expanded ST branch-based molecular evolution analyses.
To determine why accelerated rates of evolution associated with expression in the Sternorrhyncha expanded clades (Table 2), site based analyses were performed to identify the positive selected coden sites. For both the two clades, the significantly differences in the first model pairs (M0 vs. M3) indicated ω varied among all sites (Table 3). To search for the positive selected coden sites in the expanded sequences, two other model pairs were used. However, for both of the expanded clades, the two model pairs (M1a vs. M2a and M7 vs. M8) did not show significantly difference and no positive selected sites were identified (Table 3). The results indicated that the elevated ω we identified in the expanded clades (Table 2) resulted from relaxed selection constrained, but not the positive selected.
Table 3. Results of the B. tabaci Sternorrhyncha expanded ST site-based molecular evolution analyses.
Effects of Oral Delivery of STs dsRNA
Based on our annotation, nine BTSTs that matched the TIGRT00879 domain with scores above 237.8 were cloned (Figure S2). To investigate the function of BTSTs in B. tabaci, dsRNAs of the nine BTSTs were synthesized and separately fed to B. tabaci adults. Mortality was recorded after the adults had fed on the dsRNAs for 2 and 4 days (Table 4). Feeding on the dsRNAs significantly suppressed the expression levels of the corresponding BTSTs (Figure 6). Silencing of seven of the BTSTs (all except BTST120 and BTST134) resulted in significantly higher mortality compared to the control at day 2. However, only dsBTST40 and dsBTST44 caused significant mortality at day 4. DsBTST40 caused higher mortality than the other dsRNAs on both day 2 and 4. Mortality caused by the dsRNAs was the lowest for dsBTST134.
Table 4. Effects of silencing nine BTSTs by oral delivery of dsRNA on the mortality of adult B. tabaci.
Figure 6. Temporal profiles of RNAi effects. A total of nine BTSTs were investigated. The gene expression levels in B. tabaci adults were monitored by RT-qPCR after treating by 2 and 4 days. Statistical analysis of mRNA levels was performed with student t-test (*P < 0.05; **P < 0.01).
In our study, a total of 137 BTSTs were identified from B. tabaci MEAM1. Because of genome complexity, some redundant BTSTs exist. However, whether those duplicated BTSTs exist on different scaffolds is still uncertain. Among these identified BTSTs, for all but three of BTSTs had transcriptome coverage. Complete coding sequences of nine BTSTs that contained the TIGR00879 motif and partial coding sequences of 24 randomly selected BTSTs were also cloned successfully (Figures S2, S3 and Table S6). These results suggested that the quality of the BTSTs annotation was good. The 137 BTSTs were located on 86 scafflolds and a total of 26 gene clusters were also identified, which indicated duplication could be accounted for the expansion of BTSTs. We also anticipate that the several remaining BTST expansion members are likely located on neighboring scaffolds, which will be resolved by the improvement of B. tabaci genome in the future.
Previous studies have shown that A. pisum and B. mori contained a large ST family (Price et al., 2010; Govindaraj et al., 2016). Our study showed that B. tabaci encodes much more STs than A. pisum, B. mori, and nine other insects. Our phylogenetic analysis showed that the evolutionary pattern of the ST family differed among selected lepidopterans and sternorrhynchans, which was consistent with the phylogenetic relationships of the insects. This phenomenon also consisted with the previous finding that the pattern of insect's digestion correlated well with its phylogenetic position (Terra, 1990). As noted earlier, STs mediate the transport of sugar into or out of cells. Furthermore, the sugar content of food, feeding behavior, and digestion differ among sternorrhynchans (like B. tabaci and A. pisum) and lepidopterans (like B. mori and M. sexta) (Terra, 1990; Ashford et al., 2000; Douglas, 2006). A recent study also revealed that the divergent evolutionary pattern of STs is associated with the difference in sugar accumulation between grasses and eudicots (Wang et al., 2016). Thus, the different evolutionary patterns of STs in different insects may result from differences in food quantity, suck-feeding behavior, and digestion. The Diptera expanded clade grouped with one of the Lepidoptera expanded clades, perhaps because lepidopterans are phylogenetically close to dipterans (Misof et al., 2014). In addition, phylogenetic analysis showed that B. tabaci had 68 STs more than A. pisum, while it had 63 STs more than A. pisum in the expanded clades, which suggesting that most of the difference in number of STs in B. tabaci and A. pisum was accounted for by STs in expanded clades.
Although predicting the function of STs based on the similarity of amino acid sequences is difficult (Kikuta et al., 2012), the expression level of STs provides clue about their functional role. Using gene expression data, previous studies have revealed the roles of STs in sugar accumulation in plants (Reuscher et al., 2014; Li et al., 2015). In aphids and planthoppers, several gut-specific STs were identified based on expression data (Kikuta et al., 2010; Price and Gatehouse, 2014). For B. tabaci, BTSTs were divided into three groups based on their expression levels. The expressional pattern of group 1 indicates that those BTSTs play vital roles in B. tabaci development, because B. tabaci does not feed in the egg stage. Some of these BTSTs in group 2 may be involved in feeding or post-egg development. BTSTs in group 3 were expressed weakly across all stages or were only expressed in one or two stages. Interestingly, among the 17 BTSTs that contained fewer than 12 transmembrane domains, 12 of them were assigned to group 3. The 12-transmembrane structure has been demonstrated to be important for ST function (Pazdernik et al., 1997; Yan, 2015). Loss of transmembrane domains may lead to reduced or no expression of STs. The lower expression pattern and fewer transmembrane domains of 12 BTSTs in group 3 indicate that they have probably lost their functions. Expression profiles showed that nearly all of the BTSTs were expressed at a higher level in nymphs than adults. This is probably because B. tabaci nymphs develop rapidly and store nutrition for molting. Finally, the transcriptome data from our recent study (Xie et al., 2014) in which female and male adults of B. tabaci which were collected from different host plants showed that the expression patterns of BTSTs were clustered based on sex rather than on host plant. The differences in the expression of BTSTs between females and males, may be caused by differences in the requirements for sugars by females and males. Because B. tabaci has a wide range of host plants that likely contain different concentrations of sugar in their phloem, these results indicate that B. tabaci has probably evolved a highly effective sugar transport system.
Previous study also showed the expression profiles between or among duplicated genes were different (Zhang, 2003) and amino acid transporters and the slimfast amino acid transporters exhibited male-biased expression in aphid (Duncan et al., 2011; Price et al., 2011). In our study, the expression between or among several duplicated genes, such as BTST41 and BTST42, BTST10 to BTST14, and BTST67 to BTST69 in expanded clade 1 and BTST23 and BTST24, BTST93 to BTST95 in clade 2 were different. Those expressional differences of the duplicated genes were perhaps resulted from the evolution of their cis-regulatory regions and could lead to the functional diversity of the duplicated genes (Nowak et al., 1997; Wagner, 2000). To investigate whether BTSTs in Sternorrhyncha expanded clades had accelerated evolution rates associated with its expression profiles and to determine why, we performed a series of molecular evolution studies. Results of branch-based tests showed that the accelerated evolution of BTSTs in the expanded clades related with their expression profiles. Subsequent site-based tests suggested that the accelerated rate of evolution probably resulted from relaxed selection constaint. Sequence number, sequence length, and sequence divergence will influence the finding of positive selection sites (Anisimova et al., 2001). Because the sequences varied and each analysis involved massive numbers of sequences, perhaps these factors may explain the failure to identify positive selection sites. However, previous studies also detected relaxed selection constaint in amino acid transporters from slimfast-expanded clades of A. pisum (Price et al., 2011). Relaxed selection constraint could maintain duplicated genes by complementary degenerative mutations. To fulfill the complete function of the parent gene, each of the duplicated genes could not be removed (Force et al., 1999). Relaxed selection constraint could also cause the functional diversity of duplicate genes by fixed mutation in one daughter gene. The fixed mutation could lead to subfunctionalization of the daughter gene when the environment or the genetic group changed (Zhang, 2003). In addition, relaxed selection constraint could lead to new form of biased expression (Hunt et al., 2011). So, the accelerated rate of evolution probably resulted from relaxed selection constaint the relaxed selection constraint. For expanded genes, the different expression profiles, and the relaxed selection constraint indicated that those duplicated BTSTs may have different functions. Apart from transporting sugars as part of normal cell metabolism, STs also participate in other biological processes in insects. Under desiccation or elevated temperatures, the silencing of a trehalose transporter reduced the survival of A. gambiae (Liu et al., 2013). Sugar transporters were also reported to play a role in interactions between insects and pathogens (Dussaubat et al., 2012). As an invasive and polyphagous pest, B. tabaci is confronted with various biotic and abiotic stresses; therefore, the expanded BTSTs may help B. tabaci endure these stresses.
Pervious study reported that candidate gut ApSTs which contained TIGR00879 motif transported glucose in A. pisum (Price et al., 2010). Later, another studies showed silencing candidate gut MpST which contained TIGR00879 motif increased hemolymph osmotic pressure in M. persicae (Tzin et al., 2015). As osmoregulation mechanism is vital important for B. tabaci survive, silencing the genes in osmoregulation mechanism could be used for controlling B. tabaci. In this study, a total of nine BTSTs which contained TIGR00879 motif were chosen to investigate the possibility of using STs as RNAi target for whitefly control. All the genes were expressed across the whole developmental stages; with BTST40 and BTST44 in group 2 were low expressed at the egg stage. The results showed that silencing seven of these BTSTs could significantly reduce the survival of B. tabaci. Compared with silencing BTST40 and BTST44, silencing five of these BTSTs including BTST45, BTST50, BTST81, BTST107, and BTST111 can only significantly increases the mortality rate of B. tabaci at day 2. One possible explanation for the differences in mortality rate was perhaps these five BTSTs were not involved in regulating osmotic pressure. Another possibility may result from influencing the normal metabolism upon silencing at 2 days and then the functions of the five BTSTs were accomplished by other BTSTs. Silencing the BTST40 and BTST44 significantly increasing the mortality rate of B. tabaci at day 2 and 4. Interestingly, based on their expression, BTST45, BTST81, BTST107, and BTST111 were divided into group 1, BTST50 was divided into group 3, while BTST40 and BTST44 were listed in group 2. It seems that the silencing effect were associated with the expression group (gene expression values) (Figure 2). As B. tabaci did not feed at egg stage and almost all genes in group 2 did not expressed at egg stages, genes in group 2 were assumed to involve in feeding. The expression profiles and silencing effects of BTST40 and BTST44 in group 2 suggested that these two genes may be used as potential targets for controlling B. tabaci. Other studies showed that silencing N. lugens or A. pisum sugar transporters were harmful to insects, such as reduced the survival of N. lugens nymphs (Zha et al., 2011; Ge et al., 2015) and reduced the fecundity of A. pisum (Tzin et al., 2015). The current and previous results indicate that the silencing of STs could be used to control of phloem-feeding insects. To find the suitable STs for whitefly biocontrol, much more work, such as biochemistry analysis, function analysis and other detailed expressional analysis, still needs to be performed.
In this study, a genomic-wide identification and expression analysis of BTSTs was performed based on genome and transcriptome datasets. Comparative analysis of BTSTs and STs in other insects showed that B. tabaci encodes an expanded ST family. Furthermore, molecular analysis suggested that the expanded clades of BTSTs have an accelerate rate of evolution, and the accelerate rate of evolution is consistent with the BTSTs expression profiles. Additionally, BTST40 and BTST44 were identified as potential target genes for B. tabaci control. In short, our study presents a global view of BTSTs and provides a starting point for further research on the functions of STs in B. tabaci.
YZ and ZY conceived and designed the experiment; ZY and JX performed the experiment; ZY, CG, and HZ analyzed the data; WX, ZG, SW, XY, FY, and QW contributed reagents/materials/analysis tools; ZY drafted the paper; YZ and HP edited the manuscript; YZ supervised the entire project.
This work was funded by the National Natural Science Foundation of China (31420103919, 31572014), China Agriculture Research System (CARS-26-10), Beijing Training Project for the Leading Talents in S & T (LJRC201412), and the Beijing Key Laboratory for Pest Control and Sustainable Cultivation of Vegetables.
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 Supplementary Material for this article can be found online at: https://www.frontiersin.org/article/10.3389/fphys.2017.00322/full#supplementary-material
ST, sugar transporter; BTST, B. tabaci sugar transporter; mtCOI, mitochondria cytochrome oxidase one; FPKM, fragments per kilobase of exon model per million fragments mapped; RNAi, RNA interference; dsRNA, double-stranded RNA; MFS, major facilitator superfamily.
Altschul, S. F., Madden, T. L., Schaffer, A. A., Zhang, J., Zhang, Z., Miller, W., et al. (1997). Gapped BLAST and PSI-BLAST: a new generation of protein database search programs. Nucleic Acids Res. 25, 3389–3402. doi: 10.1093/nar/25.17.3389
Anisimova, M., Bielawski, J. P., and Yang, Z. (2001). Accuracy and power of the likelihood ratio test in detecting adaptive molecular evolution. Mol. Biol. Evol. 18, 1585–1592. doi: 10.1093/oxfordjournals.molbev.a003945
Ashford, D. A., Smith, W. A., and Douglas, A. E. (2000). Living on a high sugar diet: the fate of sucrose ingested by a phloem-feeding insect, the pea aphid Acyrthosiphon pisum. J. Insect Physiol. 46, 335–341. doi: 10.1016/S0022-1910(99)00186-9
Boykin, L. M., and De Barro, P. J. (2014). A practical guide to identifying members of the Bemisia tabaci species complex: and other morphologically identical species. Front. Ecol. Evol. 2:45. doi: 10.3389/fevo.2014.00045
Byrne, D. N., and Miller, W. B. (1990). Carbohydrate and amino acid composition of phloem sap and honeydew produced by Bemisia tabaci. J. Insect Physiol. 36, 433–439. doi: 10.1016/0022-1910(90)90061-J
Capella-Gutierrez, S., Silla-Martinez, J. M., and Gabaldon, T. (2009). TrimAl: a tool for automated alignment trimming in large-scale phylogenetic analyses. Bioinformatics 25, 1972–1973. doi: 10.1093/bioinformatics/btp348
Chu, D., Wan, F. H., Zhang, Y. J., and Brown, J. K. (2010). Change in the biotype composition of Bemisia tabaci in Shandong Province of China from 2005 to 2008. Environ. Entomol. 39, 1028–1036. doi: 10.1603/EN09161
Chu, D., Zhang, Y. J., Brown, J. K., Cong, B., Xu, B. Y., Wu, Q. J., et al. (2006). The introduction of the exotic Q biotype of Bemisia tabaci from the mediterranean region into China on ornamental crops. Fla. Entomol. 89, 168–174. doi: 10.1653/0015-4040(2006)89[168:TIOTEQ]2.0.CO;2
Cristofoletti, P. T., Ribeiro, A. F., Deraison, C., Rahbe, Y., and Terra, W. R. (2003). Midgut adaptation and digestive enzyme distribution in a phloem feeding insect, the pea aphid Acyrthosiphon pisum. J. Insect Physiol. 49, 11–24. doi: 10.1016/S0022-1910(02)00222-6
Doidy, J., Grace, E., Kühn, C., Simon-Plas, F., Casieri, L., and Wipf, D. (2012). Sugar transporters in plants and in their interactions with fungi. Trends Plant Sci. 17, 413–422. doi: 10.1016/j.tplants.2012.03.009
Duncan, R. P., Nathanson, L., and Wilson, A. C. (2011). Novel male-biased expression in paralogs of the aphid slimfast nutrient amino acid transporter expansion. BMC Evol. Biol. 11:253. doi: 10.1186/1471-2148-11-253
Dussaubat, C., Brunet, J. L., Higes, M., Colbourne, J. K., Lopez, J., Choi, J. H., et al. (2012). Gut pathology and responses to the microsporidium Nosema ceranae in the honey bee Apis mellifera. PLoS ONE 7:e37017. doi: 10.1371/journal.pone.0037017
Finn, R. D., Coggill, P., Eberhardt, R. Y., Eddy, S. R., Mistry, J., Mitchell, A. L., et al. (2016). The Pfam protein families database: towards a more sustainable future. Nucleic Acids Res. 44, D279–D285. doi: 10.1093/nar/gkv1344
Ge, L. Q., Jiang, Y. P., Xia, T., Song, Q. S., Stanley, D., Kuai, P., et al. (2015). Silencing a sugar transporter gene reduces growth and fecundity in the brown planthopper, Nilaparvata lugens (Stal) (Hemiptera: Delphacidae). Sci. Rep. 5:12194. doi: 10.1038/srep12194
Govindaraj, L., Gupta, T., Esvaran, V. G., Awasthi, A. K., and Ponnuvel, K. M. (2016). Genome-wide identification, characterization of sugar transporter genes in the silkworm Bombyx mori and role in Bombyx mori nucleopolyhedrovirus (BmNPV) infection. Gene 579, 162–171. doi: 10.1016/j.gene.2015.12.057
Haas, B. J., Papanicolaou, A., Yassour, M., Grabherr, M., Blood, P. D., Bowden, J., et al. (2013). De novo transcript sequence reconstruction from RNA-seq using the Trinity platform for reference generation and analysis. Nat. Protocols 8, 1494–1512. doi: 10.1038/nprot.2013.084
Haft, D. H., Loftus, B. J., Richardson, D. L., Yang, F., Eisen, J. A., Paulsen, I. T., et al. (2001). TIGRFAMs: a protein family resource for the functional identification of proteins. Nucleic Acids Res. 29, 41–43. doi: 10.1093/nar/29.1.41
Hansen, A. K., and Moran, N. A. (2011). Aphid genome expression reveals host-symbiont cooperation in the production of amino acids. Proc. Natl. Acad. Sci. U.S.A. 108, 2849–2854. doi: 10.1073/pnas.1013465108
Huang, H. T., Leu, J. H., Huang, P. Y., and Chen, L. L. (2012). A putative cell surface receptor for white spot syndrome virus is a member of a transporter superfamily. PLoS ONE 7:e33216. doi: 10.1371/journal.pone.0033216
Hunt, B. G., Ometto, L., Wurm, Y., Shoemaker, D., Yi, S. V., Keller, L., et al. (2011). Relaxed selection is a precursor to the evolution of phenotypic plasticity. Proc. Natl. Acad. Sci. U.S.A. 108, 15936–15941. doi: 10.1073/pnas.1104825108
Katoh, K., Misawa, K., Kuma, K., and Miyata, T. (2002). MAFFT: a novel method for rapid multiple sequence alignment based on fast Fourier transform. Nucleic Acids Res. 30, 3059–3066. doi: 10.1093/nar/gkf436
Kikawada, T., Saito, A., Kanamori, Y., Nakahara, Y., Iwata, K., Tanaka, D., et al. (2007). Trehalose transporter 1, a facilitated and high-capacity trehalose transporter, allows exogenous trehalose uptake into cells. Proc. Natl. Acad. Sci. U.S.A. 104, 11585–11590. doi: 10.1073/pnas.0702538104
Kikuta, S., Hagiwara-Komoda, Y., Noda, H., and Kikawada, T. (2012). A novel member of the trehalose transporter family functions as an H+-dependent trehalose transporter in the reabsorption of trehalose in malpighian tubules. Front. Physiol. 3:290. doi: 10.3389/fphys.2012.00290
Kikuta, S., Kikawada, T., Hagiwara-Komoda, Y., Nakashima, N., and Noda, H. (2010). Sugar transporter genes of the brown planthopper, Nilaparvata lugens: a facilitated glucose/fructose transporter. Insect Biochem. Mol. Biol. 40, 805–813. doi: 10.1016/j.ibmb.2010.07.008
Kikuta, S., Nakamura, Y., Hattori, M., Sato, R., Kikawada, T., and Noda, H. (2015). Herbivory-induced glucose transporter gene expression in the brown planthopper, Nilaparvata lugens. Insect Biochem. Mol. Biol. 64, 60–67. doi: 10.1016/j.ibmb.2015.07.015
Li, J., Zheng, D., Li, L. T., Qiao, X., Wei, S., Bai, B., et al. (2015). Genome-wide function, evolutionary characterization and expression analysis of sugar transporter family genes in pear (Pyrus bretschneideri Rehd). Plant Cell Physiol. 56, 1721–1737. doi: 10.1093/pcp/pcv090
Li, R., Xie, W., Wang, S., Wu, Q., Yang, N., Yang, X., et al. (2013). Reference gene selection for qRT-PCR analysis in the sweetpotato whitefly, Bemisia tabaci (Hemiptera: Aleyrodidae). PLoS ONE 8:e53006. doi: 10.1371/journal.pone.0053006
Liu, K., Dong, Y., Huang, Y., Rasgon, J. L., and Agre, P. (2013). Impact of trehalose transporter knockdown on Anopheles gambiae stress adaptation and susceptibility to Plasmodium falciparum infection. Proc. Natl. Acad. Sci. U.S.A. 110, 17504–17509. doi: 10.1073/pnas.1316709110
Liu, S. S., Colvin, J., and De Barro, P. J. (2012). Species concepts as applied to the whitefly Bemisia tabaci systematics: how many species are there? J. Integr. Agr. 11, 176–186. doi: 10.1016/S2095-3119(12)60002-1
Manel, N., Kim, F. J., Kinet, S., Taylor, N., Sitbon, M., and Battini, J. L. (2003). The ubiquitous glucose transporter GLUT-1 is a receptor for HTLV. Cell 115, 449–459. doi: 10.1016/S0092-8674(03)00881-X
Misof, B., Liu, S., Meusemann, K., Peters, R. S., Donath, A., Mayer, C., et al. (2014). Phylogenomics resolves the timing and pattern of insect evolution. Science 346, 763–767. doi: 10.1126/science.1257570
Pan, H., Chu, D., Ge, D., Wang, S., Wu, Q., Xie, W., et al. (2011). Further spread of and domination by Bemisia tabaci (Hemiptera: Aleyrodidae) biotype Q on field crops in China. J. Econ. Entomol. 104, 978–985. doi: 10.1603/EC11009
Pan, H., Chu, D., Yan, W., Su, Q., Liu, B., Wang, S., et al. (2012a). Rapid spread of Tomato yellow leaf curl virus in China is aided differentially by two invasive whiteflies. PLoS ONE 7:e34817. doi: 10.1371/journal.pone.0034817
Pan, H., Li, X., Ge, D., Wang, S., Wu, Q., Xie, W., et al. (2012b). Factors affecting population dynamics of maternally transmitted endosymbionts in Bemisia tabaci. PLoS ONE 7:e30760. doi: 10.1371/journal.pone.0030760
Pan, H., Preisser, E. L., Chu, D., Wang, S., Wu, Q., Carrière, Y., et al. (2015). Insecticides promote viral outbreaks by altering herbivore competition. Ecol. Appl. 25, 1585–1595. doi: 10.1890/14-0752.1
Pazdernik, N. J., Cain, S. M., and Brooker, R. J. (1997). An analysis of suppressor mutations suggests that the two halves of the lactose permease function in a symmetrical manner. J. Biol. Chem. 272, 26110–26116. doi: 10.1074/jbc.272.42.26110
Price, D. R., Duncan, R. P., Shigenobu, S., and Wilson, A. C. (2011). Genome expansion and differential expression of amino acid transporters at the aphid/Buchnera symbiotic interface. Mol. Biol. Evol. 28, 3113–3126. doi: 10.1093/molbev/msr140
Price, D. R., Karley, A. J., Ashford, D. A., Isaacs, H. V., Pownall, M. E., Wilkinson, H. S., et al. (2007a). Molecular characterisation of a candidate gut sucrase in the pea aphid, Acyrthosiphon pisum. Insect Biochem. Mol. Biol. 37, 307–317. doi: 10.1016/j.ibmb.2006.12.005
Price, D. R., Tibbles, K., Shigenobu, S., Smertenko, A., Russell, C. W., Douglas, A. E., et al. (2010). Sugar transporters of the major facilitator superfamily in aphids; from gene prediction to functional characterization. Insect Mol. Biol. 19(Suppl. 2), 97–112. doi: 10.1111/j.1365-2583.2009.00918.x
Price, D. R., Wilkinson, H. S., and Gatehouse, J. A. (2007b). Functional expression and characterisation of a gut facilitative glucose transporter, NlHT1, from the phloem-feeding insect Nilaparvata lugens (rice brown planthopper). Insect Biochem. Mol. Biol. 37, 1138–1148. doi: 10.1016/j.ibmb.2007.07.001
Reuscher, S., Akiyama, M., Yasuda, T., Makino, H., Aoki, K., Shibata, D., et al. (2014). The sugar transporter inventory of tomato: genome-wide identification and expression analysis. Plant Cell Physiol. 55, 1123–1141. doi: 10.1093/pcp/pcu052
Sagisaka, A., Fujita, K., Nakamura, Y., Ishibashi, J., Noda, H., Imanishi, S., et al. (2010). Genome-wide analysis of host gene expression in the silkworm cells infected with Bombyx mori nucleopolyhedrovirus. Virus Res. 147, 166–175. doi: 10.1016/j.virusres.2009.10.015
Schroeder, J. I., Delhaize, E., Frommer, W. B., Guerinot, M. L., Harrison, M. J., Herrera-Estrella, L., et al. (2013). Using membrane transporters to improve crops for sustainable food production. Nature 497, 60–66. doi: 10.1038/nature11909
Trapnell, C., Roberts, A., Goff, L., Pertea, G., Kim, D., Kelley, D. R., et al. (2012). Differential gene and transcript expression analysis of RNA-seq experiments with TopHat and Cufflinks. Nat. Protoc. 7, 562–578. doi: 10.1038/nprot.2012.016
Tzin, V., Yang, X., Jing, X., Zhang, K., Jander, G., and Douglas, A. E. (2015). RNA interference against gut osmoregulatory genes in phloem-feeding insects. J. Insect Physiol. 79, 105–112. doi: 10.1016/j.jinsphys.2015.06.006
Wagner, A. (2000). Decoupled evolution of coding region and mRNA expression patterns after gene duplication: implications for the neutralist-selectionist debate. Proc. Natl. Acad. Sci. U.S.A. 97, 6579–6584. doi: 10.1073/pnas.110147097
Wang, W., Zhou, H., Ma, B. Q., Owiti, A., Korban, S. S., and Han, Y. P. (2016). Divergent evolutionary pattern of sugar transporter genes is associated with the difference in sugar accumulation between grasses and eudicots. Sci. Rep. 6:29153. doi: 10.1038/srep29153
Xie, W., Wu, Q., Wang, S., Jiao, X., Guo, L., Zhou, X., et al. (2014). Transcriptome analysis of host-associated differentiation in Bemisia tabaci (Hemiptera: Aleyrodidae). Front. Physiol. 5:487. doi: 10.3389/fphys.2014.00487
Yang, X., He, C., Xie, W., Liu, Y., Xia, J., Yang, Z., et al. (2016). Glutathione S-transferases are involved in thiamethoxam resistance in the field whitefly Bemisia tabaci Q (Hemiptera: Aleyrodidae). Pestic. Biochem. Physiol. 134, 73–78. doi: 10.1016/j.pestbp.2016.04.003
Zha, W., Peng, X., Chen, R., Du, B., Zhu, L., and He, G. (2011). Knockdown of midgut genes by dsRNA-transgenic plant-mediated RNA interference in the hemipteran insect Nilaparvata lugens. PLoS ONE 6:e20504. doi: 10.1371/journal.pone.0020504
Keywords: B. tabaci, sternorrhynchan insect, sugar transporter, phylogenetic analysis, expression pattern
Citation: Yang Z, Xia J, Pan H, Gong C, Xie W, Guo Z, Zheng H, Yang X, Yang F, Wu Q, Wang S and Zhang Y (2017) Genome-Wide Characterization and Expression Profiling of Sugar Transporter Family in the Whitefly, Bemisia tabaci (Gennadius) (Hemiptera: Aleyrodidae). Front. Physiol. 8:322. doi: 10.3389/fphys.2017.00322
Received: 11 February 2017; Accepted: 03 May 2017;
Published: 23 May 2017.
Edited by:Fernando Ariel Genta, Oswaldo Cruz Foundation, Brazil
Reviewed by:Denis Tagu, Institut National de la Recherche Agronomique (INRA), France
Bruno Gomes, Liverpool School of Tropical Medicine, United Kingdom
Kexin Li, University of Haifa, Israel
Copyright © 2017 Yang, Xia, Pan, Gong, Xie, Guo, Zheng, Yang, Yang, Wu, Wang and Zhang. 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: Youjun Zhang, email@example.com
†These authors have contributed equally to this work.