Original Research ARTICLE
Bayesian phylogeny of sucrose transporters: ancient origins, differential expansion and convergent evolution in monocots and dicots
- 1Institute of Bioinformatics, University of Georgia, Athens, GA, USA
- 2Warnell School of Forestry and Natural Resources, University of Georgia, Athens, GA, USA
- 3Department of Genetics, University of Georgia, Athens, GA, USA
- 4Department of Plant Biology, University of Georgia, Athens, GA, USA
Sucrose transporters (SUTs) are essential for the export and efficient movement of sucrose from source leaves to sink organs in plants. The angiosperm SUT family was previously classified into three or four distinct groups, Types I, II (subgroup IIB), and III, with dicot-specific Type I and monocot-specific Type IIB functioning in phloem loading. To shed light on the underlying drivers of SUT evolution, Bayesian phylogenetic inference was undertaken using 41 sequenced plant genomes, including seven basal lineages at key evolutionary junctures. Our analysis supports four phylogenetically and structurally distinct SUT subfamilies, originating from two ancient groups (AG1 and AG2) that diverged early during terrestrial colonization. In both AG1 and AG2, multiple intron acquisition events in the progenitor vascular plant established the gene structures of modern SUTs. Tonoplastic Type III and plasmalemmal Type II represent evolutionarily conserved descendants of AG1 and AG2, respectively. Type I and Type IIB were previously thought to evolve after the dicot-monocot split. We show, however, that divergence of Type I from Type III SUT predated basal angiosperms, likely associated with evolution of vascular cambium and phloem transport. Type I SUT was subsequently lost in monocots along with vascular cambium, and independent evolution of Type IIB coincided with modified monocot vasculature. Both Type I and Type IIB underwent lineage-specific expansion. In multiple unrelated taxa, the newly-derived SUTs exhibit biased expression in reproductive tissues, suggesting a functional link between phloem loading and reproductive fitness. Convergent evolution of Type I and Type IIB for SUT function in phloem loading and reproductive organs supports the idea that differential vascular development in dicots and monocots is a strong driver for SUT family evolution in angiosperms.
Sucrose is among the most abundant photoassimilates and the principal transport form of carbohydrates in many plants. The intracellular movement and long-distance transport of sucrose are mediated by sucrose transporters (SUTs), a group of transmembrane proteins belonging to the major facilitator superfamily (Sauer, 2007; Ayre, 2011). SUTs are proton-coupled symporters that transport sucrose either intercellularly across plasma membranes or intracellularly from the vacuole to the cytoplasm (reviewed in Kühn and Grof, 2010; Ayre, 2011). SUTs are encoded by small gene families in all plant species analyzed to date, from the primitive land plants Physcomitrella and Selaginella (Lalonde and Frommer, 2012; Reinders et al., 2012) to the woody perennial Populus (Payyavula et al., 2011). SUT genes are expressed throughout the plant body, with varying tissue- or cell-specificity depending on the isoform function. For instance, SUT genes involved in phloem loading have been localized to the companion cells and sieve elements (Riesmeier et al., 1993; Stadler et al., 1995; Truernit and Sauer, 1995), while those involved in sucrose uptake and other sink functions were preferentially expressed in tissues like pollen (Lemoine et al., 1999; Stadler et al., 1999), root (Flemetakis et al., 2003) or xylem (Decourteix et al., 2006). The various functions are also dictated by the differential (plasma or vacuolar) membrane localization of SUT proteins.
Several studies have reported on the phylogenetic organization of the plant SUT family, though with inconsistent and sometimes confusing nomenclature (Table 1). SUT genes were initially classified into three phylogenetic groups (Type I to Type III) based on experimentally characterized members and the full complement of the SUT families from Arabidopsis and Oryza (rice) (Aoki et al., 2003, 2012; Kühn, 2003; Lalonde et al., 2004; Shiratake, 2007; Zhou et al., 2007; Lalonde and Frommer, 2012). With the growing number of SUT genes identified, especially from the grasses, four distinct phylogenetic groups (Group 1 to Group 4) became evident, with Group 1 being monocot-specific (Sauer, 2007). This classification has been adopted in several subsequent studies (Braun and Slewinski, 2009; Payyavula et al., 2011), though again with inconsistent naming (Kühn and Grof, 2010; Doidy et al., 2012; Reinders et al., 2012). In two of the studies (Braun and Slewinski, 2009; Kühn and Grof, 2010), a fifth group was identified within the monocot-specific Group 1 (Table 1). For the sake of clarity, we have adhered to the nomenclature of Aoki et al. (2003) as amended by Reinders et al. (2012), with cross-referencing to the classification of Sauer (2007) (Table 1).
The eudicot-specific Type I (Group 2) is arguably the most extensively studied group, many of them have been localized to the plasma membrane and functionally associated with high-affinity sucrose uptake for phloem loading (reviewed in Sauer, 2007). The Type II group designated by Aoki et al. (2003) is split into two sub-groups in later studies (Sauer, 2007; Payyavula et al., 2011; Reinders et al., 2012). The canonical Type II (Type IIA or Group 3) contains both eudicot and monocot isoforms, whereas Type IIB (Group 1) represents the monocot-specific SUTs first reported by Sauer (2007). Several Type IIB members are plasma membrane-localized, high-affinity transporters (reviewed in Braun and Slewinski, 2009), a striking functional similarity to eudicot-specific Type I SUTs. Like Type IIB, several Type II members are also plasma membrane-localized (Barker et al., 2000; Meyer et al., 2000), but unlike Type IIB, Type II SUTs harbor an extended central cytoplasmic loop with unclear function in both eudicots and monocots (Aoki et al., 2003; Barth et al., 2003; Meyer et al., 2004; Hackel et al., 2006). Type III (Group 4) consists of all known tonoplast SUTs from both monocots and eudicots that are thought to facilitate sucrose release from vacuoles (Eom et al., 2011; Payyavula et al., 2011; Schneider et al., 2012). Dual (tonoplast and plasma membrane) localization has been reported for some Type III members (Chincinska et al., 2013). Phylogenetically distinct SUT orthologs are also found in lower vascular (Selaginella, spikemoss) and non-vascular (Physcomitrella, moss) plants (Lalonde and Frommer, 2012; Reinders et al., 2012), suggesting their divergence early during land plant evolution.
Given the essential roles of plasma membrane SUTs in apoplastic phloem loading (Gottwald et al., 2000; Scofield et al., 2002; Slewinski et al., 2009), the independent occurrence of two monophyletic SUT groups in eudicots (Type I) and monocots (Type IIB) with similar functions is intriguing. Because Type I is absent in monocots and lower plants, Reinders et al. (2012) proposed that this class evolved after the divergence of monocots and dicots. However, the taxonomic coverage lacked representation of basal angiosperm lineages to more properly infer the evolutionary history of SUT family in flowering plants. Here, we took advantage of the rapidly growing genomic resources to reconstruct a SUT phylogeny with 41 sequenced plants and 233 gene models using the Bayesian approach with the Markov chain Monte Carlo algorithm (Ronquist et al., 2012). In addition to algae, moss and spikemoss, we included Phoenix dactylifera (date palm, Al-Dous et al., 2011) and Musa acuminate (banana, D'Hont et al., 2012) that are basal to six genome-sequenced monocots, Aquilegia coerulea (Kramer, 2009) that is basal to 28 eudicots, and Amborella trichopoda that is basal to all sequenced angiosperms (Amborella Genome Project, 2013). This was instrumental for clarifying the evolutionary history of modern SUT families and their association with key developmental innovations in angiosperm evolution.
Materials and Methods
Collection and Curation of SUT Sequences
SUT sequences from sequenced plant genomes were obtained from Phytozome v9.1, with the exceptions of Amborella trichopoda v1.0 (http://www.amborella.org), Cicer arietinum v1.0 (http://www.comparative-legumes.org), Lotus japonicas v2.5 (http://www.kazusa.or.jp/lotus), Medicago truncatula (Doidy et al., 2012 and cross-referenced with Phytozome v10), Musa acuminate v1 (http://banana-genome.cirad.fr) and Phoenix dactylifera v3 (http://qatar-weill.cornell.edu/research/datepalmGenome/download.html). The predicted gene models were subjected to manual curation to correct for gene structure prediction errors, such as miss-annotated splice junctions, guided by preliminary sequence alignment. Sequences that were too short (<300 amino acids) or represent possible splice variants were excluded from our analysis. SUT orthologs from Galdieria sulphuraria (red alga, http://genomics.msu.edu/galdieria), Cyanidioschyzon merolae (red alga, http://merolae.biol.s.u-tokyo.ac.jp), Ostreococcus lucimarinus and Ostreococcus tauri (green algae, http://genome.jgi-psf.org) were obtained using all higher plant SUT amino acid sequences as query to blast against the predicted protein databases of these species. Blast hits with >60% coverage of at least one query sequence was retained and manually inspected. This led to the identification of one homolog in C. merolae, five in G. sulphuraria, and two each in the green algae O. lucimarinus and O. tauri. No SUT homolog was found in Chlamydomonas reinhardtii or Volvox carteri green alga as reported previously (Reinders et al., 2012). Our pilot phylogenetic analysis showed that the green and red algal SUTs clustered together and joined all other plant SUTs in a single long branch, suggesting that algal SUTs can be used as outgroup. To reduce sequence divergence in multiple sequence alignment, only SUTs from red alga G. sulphuraria were included in subsequence analyses. The full list of 233 SUT gene models used in this study is provided in Supplemental Table 1. Exon-intron structures based on curated sequences of representative species were displayed using the Gene Structure Draw program (http://www.bioinformatics.uni-muenster.de/tools/strdraw).
Sequence Alignment and Phylogenetic Tree Inference
Multiple sequence alignment was performed using MAFFT 7.037 (Katoh and Standley, 2013), with the “auto” option for alignment strategy selection. The resulting alignment was manually edited using alignment viewer in MEGA 5.2 (Tamura et al., 2011). Sites consisting of mostly gaps were removed. Pairwise sequence identity matrix was calculated by Clustal2.1 using default parameters. Bayesian inference of SUT phylogeny was performed using MrBayes v3.2.1 (Ronquist et al., 2012) executed on XSEDE (Extreme Science and Engineering Discovery Environment) through the CIPRES Science Gateway v3.3 (Miller et al., 2010). We performed pilot runs using mixed models to determine the best amino acid substitution models, and the “Jones” amino acid substitution model was chosen for subsequent runs. The likelihood model parameters were Rates = gamma, Ngammacat = 8, and Covarion = no. The Markov Chain Monte Carlo parameters were: Ngen = 12000000, nruns = 2, nchains = 8, Markov chain samplefreq = 200, and burn-in fraction = 0.5. Convergence was determined by 8750 post burn-in samples from two independent runs. The resulting phylogenetic reconstruction was converted to Newick format using Phylogeny.fr (Dereeper et al., 2008) and imported into MEGA5.2 for tree rendering. Maximum Likelihood analysis was also performed and returned similar results. We focus our discussion on the results from the Bayesian analyses since the Markov chain Monte Carlo search provides a statistically rigorous characterization of the distribution of plausible tree topologies, branch lengths and substitution model parameters given the sequence alignments (Holder and Lewis, 2003).
Estimation of Selection Pressure
SUT nucleotide sequences were aligned using codon alignment option in MUSCLE implemented in MEGA 5.2. The resultant alignment was manually edited using alignment viewer in MEGA 5.2. Codon sites consisting of mostly gaps or with excessive diversity were removed. Maximum likelihood analysis of the ratio of non-synonymous and synonymous nucleotide substitution rates (ω = dN/dS) was conducted using PAML 4.5 (Yang, 2007). Modified branch site-model A (test of positive selection, model = 2, NS sites = 2) (Zhang et al., 2005) was used to test for positive selection for branches of interest from the SUT phylogeny. The likelihood was compared to a NULL model, in which foreground ω2 was fixed to 1. Likelihood ratio tests were conducted with df = 1. Bayes Empirical Bayes (BEB) analysis (Yang et al., 2005) was used to identify amino acid positions with high posterior possibility of being positively selected. To assess selection pressure of Type II and Type IIB SUTs, the edited alignment from above was divided into windows of 100 codons for dN and dS estimation using KaKs_Calculator 1.2 (Zhang et al., 2006). For Ks estimation of duplicated gene pairs, a custom perl script was written to batch-process Ks calculation using LWL method implemented in KaKs_Calculator 1.2 with coding sequence alignment results from MACSE v220.127.116.11 (Ranwez et al., 2011).
Gene Expression Analysis
Affymetrix microarray data from vegetative and reproductive tissues of O. sativa L. ssp. japonica (Fujita et al., 2010; Kudo et al., 2013) and Arabidopsis thaliana (Schmid et al., 2005; Qin et al., 2009) were obtained from NCBI GEO (GSE14304, GSE41556, GSE19024, GSE29080, GSE5629-GSE5634, and GSE17343). The probe-set expression values were extracted by MAS5 using affy package from Bioconductor (Gautier et al., 2004). For soybean gene expression analysis, published RNA-Seq data (Hunt et al., 2011; Kim et al., 2011) and three seed datasets from the Goldberg laboratory (GSE29134, GSE29162 and GSE29163) were used. The single-end 75-bp reads were filtered to remove low-quality sequences using SolexaQA DynamicTrim (Cox et al., 2010) with default settings, and searched against the SILVA rRNA database (Quast et al., 2013), plant long non-coding RNA database (PLncDB, Jin et al., 2013), Rfam non-coding RNA database (Burge et al., 2013), and chloroplast (Saski et al., 2005) and mitochondrial genomes (Chang et al., 2013) to remove contaminants. The pre-processed reads were mapped to Glycine max v1.1 genome (Schmutz et al., 2010) using Tophat 2.0.10 (Trapnell et al., 2012). Only uniquely mapped reads were used to assess transcript abundance in reads per kilobase per million using cufflinks 2.1.1 (Trapnell et al., 2012). Expression values were normalized by Z-score transformation (Cheadle et al., 2003; Schmid et al., 2005) and visualized in heat maps using pheatmap package in R.
Modern SUT Gene Family Evolved from Two Ancient Groups
The SUT phylogenetic tree inferred from the Bayesian method has strong support for the major nodes (Figure 1). The tree revealed two major clades for land plant SUTs, each with two previously recognized SUT groups—an overall topology similar to that reported elsewhere (Sauer, 2007; Braun and Slewinski, 2009; Payyavula et al., 2011; Doidy et al., 2012; Reinders et al., 2012). The smaller of the two clades consisted of Type II (Group 3) and Type IIB (Group 1), and the larger one comprised Type I (Group 2) and Type III (Group 4) (Table 1). The algal SUTs formed a strongly supported branch distinct from the two major clades (Figure 1), similar again in topology to that reported by Payyavula et al. (2011) and Reinders et al. (2012). The strong support for the two land plant clades descending from the algal clade suggests that modern plant SUT genes evolved from two different ancestors, hereafter referred to as ancient groups AG1 and AG2. SUT homologs from primitive plants (moss and spikemoss) were found in both AG1 and AG2, suggesting that the two ancient groups diverged early in the evolutionary history of land plants. To shed light on the subsequent evolution of AG1 and AG2 into the four modern SUT groups, we reconstructed two phylogenetic trees separately for the two major clades. This clade-specific approach was expected to reduce erroneous alignment among less closely related sequences, thereby improving the inference accuracy of SUT family evolution.
Figure 1. Bayesian phylogenetic inference of SUT from 41 sequenced plant genomes. Modern angiosperm SUTs form four distinct groups (Types I, II, IIB, and III) nested in two ancient groups AG1 and AG2, using red alga (Galdieria sulphuraria) SUTs as out group. Type II and Type III represent evolutionarily conserved groups with both monocot and eudicot members, whereas Type I and Type IIB are found only in eudicots and monocots, respectively. Basal lineages are denoted in solid symbols. Posterior probabilities for major nodes are shown.
AG1 Duplication was Lost in Monocots but Retained and Expanded in Eudicots
The AG1 clade is more than twice as large as the AG2 clade (Figure 1, Supplemental Table 1). Moss and spikemoss SUTs were basal to all other angiosperm SUTs, and both taxa have independently experienced SUT gene duplication, yielding four copies each in AG1 (Figure 2A). The angiosperm SUTs formed two strongly supported groups, corresponding to the eudicot-specific Type I and monocot- and eudicot-containing Type III (Figure 2A). In both cases, the basal position was occupied by an Amborella SUT homolog, suggesting that Type I and Type III SUTs diverged very early, perhaps before the advent of angiosperms. Both Type I and Type III Amborella SUTs have the same gene (exon-intron) structure that is also conserved in angiosperm Type III, but not Type I SUTs (Figure 3). This suggests that Type I was derived from Type III and has subsequently experienced an intron loss in the progenitor angiosperm. The complete absence of Type I SUTs in monocots supports the interpretation that the progenitor Type I SUT was lost from the ancestral monocot genome. Type I SUT was also absent in the current draft genome assembly of basal eudicot Aquilegia, although a partial match to Type I SUT was found on scaffold 6 flanked by repeat elements. This suggested either a genome assembly artifact or possibly an independent gene loss event in Aquilegia. Type III monocot and eudicot SUTs formed two distinct groups, with date palm/banana and Aquilegia members occupying the respective basal position (Figure 2B). Despite its broad taxonomic representation, the Type III clade is noticeably smaller than the eudicot-only Type I clade, mainly because the vast majority of angiosperm species sampled (71%) contain a single Type III gene (Figure 2B, Supplemental Table 1). This contrasts sharply with the eudicot-specific Type I clade where most (52%) taxa contain three or more copies (Figure 2A, Supplemental Table 1), namely the Brassicaceae (i.e., Arabidopsis, Capsella, Brassica, Thellungiella), legumes (Glycine, Phaseolus, Cicer, Medicago and Lotus), Malvaceae (Theobroma and Gossypium), Linum (flax), and Fragaria (strawberry). These results suggest a greater tendency of Type I SUTs to be duplicated and retained since their split from Type III, and this trend was particularly escalated in several lineages.
Figure 2. Evolution of ancient group AG1 SUTs. (A) Bayesian phylogenetic inference of AG1 SUTs supports the divergence of Type I and Type III form progenitor Physcomitrella and Selaginella SUTs (gray diamonds). Amborella members (black squares) are basal to modern angiosperm SUTs in both cases. (B) Zoom-in view of the angiosperm Type III branch. Eudicot and monocot members form distinct groups, with Aquilegia (black circle) and Phoenix/Musa (black triangles) occupying the respective basal positions. (C) Zoom-in view of Brassicaceae Type I branch with three subclades B1, B2, and B3. (D) Zoom-in view of the legume (Fabeceae) Type I branch with three subclades F1, F2, and F3. Posterior probabilities for major nodes are shown. Sequence names are provided in Supplemental Table 1. (E) Ks estimation between subcalde members of the expanded Arabidopsis and Glycine Type I SUTs. Values are means and standard deviations of all gene pairs within each comparison group.
Figure 3. Exon-intron structure of SUT genes in representative species arranged by SUT groups. Ancient groups (AG1-AG2), Type I subclades of Brassicaceae (B1 to B3) and Fabeceae (F1 to F3), and Type IIB subclades of Poaceae (P1 to P3) are indicated. Basal lineages are denoted by solid symbols (gray diamonds, Physcomitrella (Pp) and Selaginella (Smo); black squares, Amborella (AmTr); black triangles, Phoenix (PDK). Introns are not drawn to scale, and two Phoenix gene models contain sequence gaps within the first exon. Other taxa are: Arabidopsis (At), Brachypodium (Bradi), Glycine (Gm), Oryza (Os), Populus (Potri), and Zea (Zm).
The Brassicaceae Type I members clustered into three strongly supported subclades, referred to as B1, B2, and B3 (Figure 2C). The well-characterized AtSUC2 (At1g22710), known to be involved in phloem loading (Truernit and Sauer, 1995; Gottwald et al., 2000; Srivastava et al., 2008), belongs to the small B1 clade that is basal to the expanded B2 and B3. All species were represented by a single SUT in the B1 clade, except Brassica that has experienced genome triplication. Orthologs in the B1 clade share high sequence similarities with one another (>94%), as well as conserved gene structure with the other angiosperm Type I members (Figure 3). The B2 clade contains two branches, the larger of which was similar to the B1 clade with mostly single-copy representation, including the pollen-expressing AtSUC1 (At1g71880), whereas the smaller branch contains Camelineae-specific (Arabidopsis and Capsella) tandem duplicates. The B3 clade is the largest, with 2–4 copies per species. Members of the B2 and B3 clades experienced an intron-loss event unlike the other angiosperm Type I SUTs (Figure 3). Synteny analysis based on the Plant Genome Duplication Database (Lee et al., 2012) showed that AtSUC2 (clade B1) and AtSUC1 (B2, main branch) reside in large collinear blocks that are also syntenic with many other species, whereas members of the B2 small branch and B3 clade showed no syntenic relationship outside of Brassicaceae. The B1 clade thus represents the founding member of the ancestral Brassicaceae genome. Based on Ks analysis (Figure 2E), we infer that the most recent common ancestor (MRCA) of clades B2 and B3 arose from B1 via Brassicaceae-specific alpha duplication (Bowers et al., 2003), whereas clade B3 likely originated from B2 via segmental duplications.
Similar to the Brassicaceae, the Type I SUT expansion in flax also involved multiple rounds of duplication as well as gene structure changes, including one divergent intronless member (Lus10007702, Supplemental Figure 1) that did not cluster with the other flax SUTs in the current phylogenetic tree (Figure 2A). The expansion scenario in the legumes (Fabeceae) is somewhat different, with all members retaining the conserved gene structure of angiosperm Type I SUTs (Figure 3). The legume SUTs formed three subclades (F1 to F3, Figure 2D), each with one or two members from the basal Lotus, suggesting their origin in the ancestral legume. Clade F1 appeared to be the founding group, with mostly single-copy members (except Lotus) that are highly similar to each other (87–97%). Based on Ks analysis (Figure 2E), the MRCA of clades F2 and F3 likely evolved from clade F1 via the legume-specific whole genome duplication (WGD) event (Schmutz et al., 2010). The F2 and F3 clades likely originated from a tandem duplication event in the ancestral legume shortly after the legume-specific WGD, since members in these two clades are located in tandem in both Glycine (soybean) and Phaseolus (common bean). Clade F3 members appear to be lost in Hologalegina (Cicer and Medicago) after their divergence from Millettioid (Glycine and Phaseolus). In some cases, additional lineage-specific duplications were observed (Figure 2D).
AG2 was Preferentially Expanded in Monocots, with Evidence of Positive Selection
Like in AG1, moss and spikemoss SUTs were basal to angiosperm SUTs in the AG2 tree (Figure 4A). Two tandem copies of Amborella SUTs were basal to monocot and eudicot SUTs that formed two separate branches. The monocot- and eudicot-specific clustering is notably different from the separation of Type II (Group 3, monocots and eudicots) and Type IIB (Group 1, monocots only) in previous studies (Sauer, 2007; Braun and Slewinski, 2009; Payyavula et al., 2011; Doidy et al., 2012; Reinders et al., 2012). However, the pattern is consistent with the interpretation that all monocot SUTs within AG2 descended from one MRCA, sister to the eudicot MRCA. Two sub-clades were observed within the monocot branch, each accompanied by SUT members from basal monocots date palm and banana (Figure 4A). The smaller clade includes members that were previously classified as the monocot branch of the Type II/Group 3 (Figure 4A) (Sauer, 2007; Braun and Slewinski, 2009; Payyavula et al., 2011; Reinders et al., 2012). Their inferred evolutionary distance (branch length) was similar to that of the eudicot Type II members, with conserved gene structure that is also shared by the progenitor Amborella and spikemoss SUTs (Figure 3). The larger clade corresponds to the monocot-specific Type IIB (Group I in Sauer, 2007), with much longer branch lengths. Type IIB SUTs exhibit highly variable gene structures, not conserved with Type II (Figure 3). Together, these data suggest that Type IIB arose from Type II early in monocot evolution, before the divergence of Poales (grasses), Arecales (palm) and Zingiberales (banana).
Figure 4. Evolution of ancient group AG2 SUTs. (A) Bayesian phylogenetic inference of AG2 SUTs. Physcomitrella and Selaginella members (gray diamonds) are basal to all other angiosperm SUTs. Amborella SUTs (black squares) are sister to modern angiosperm members that form eudicot- and monocot-specific branches, with Aquilegia (black circle) and Phoenix/Musa (black triangles) SUTs at the respective basal positions. Type IIB is derived from the monocot branch of Type II, forming three subclades P1, P2, and P3. The P values from the positive selection (PS) log likelihood ratio test (LRT) are shown for the major Type IIB branches. Posterior probabilities for major nodes are shown. Sequence names are provided in Supplemental Table 1. (B) Ks estimation between members of the expanded Type II/IIB SUTs in rice and maize. Values for maize are means and standard deviations of all gene pairs within each comparison group.
The Type IIB group was further expanded in grasses after their divergence from basal monocots, forming three subclades (P1, P2, and P3, Figure 4A) each represented by all six sequenced grasses (Oryza, Zea, Sorghum, Setaria, Pancium, and Brachypodium). A similar observation was reported previously, with clade P3 corresponding to the monocot-specific Group 5 designated by Braun and Slewinski (2009), or the SUT5 clade described in Kühn and Grof (2010). Interestingly, Type IIB and its three subclades all descended from their MRCAs via long branches (Figure 4A). While this may be an artifact of long branch attraction arising from limited taxon sampling (Stefanovic et al., 2004), long branches were not observed in the monocot clades of Type II (or Type III) with the same taxon coverage. This led us to suspect a rapid evolution of Type IIB SUTs. We examined the non-synonymous (dN) and synonymous (dS) substitution rates of Type IIB as well as its sister Type II members across a sliding window of 100 codons (Supplemental Figure 2). Both SUT groups showed predominantly higher dS than dN, though some regions of Type II sequences exhibited a slightly elevated dN/dS ratio. The results suggested that Type II and Type IIB SUTs are under similar levels of purifying selection, likely due to functional constraints of coding sequences. This is consistent with the short branch length within each subclade. We next tested for positive selection that might have acted on the long branches leading to the three subclades in Type IIB. Results indicated that the branches leading to clades P2 (p = 0.0002) and P3 (p = 0.02), but not P1 (p = 0.29), were indeed under positive selection (Figure 4A). Six positively selected sites in P2 and P3 members were identified by BEB analysis with a probability of >0.95, and all six mapped to an 85 amino acids region near the C-terminus. No evidence of positive selection was detected for the branches leading to the MRCA of Type IIB (p = 1), or to the MRCA of clades P1, P2 and basal monocots (p = 0.57). Positive selection might have contributed to the numerous intron-loss events, and hence hypervariable gene structures observed for P2 and P3 genes (Figure 3). Together with Ks analysis (Figure 4B), we infer that P1 is the founding clade of Type IIB, with clades P2 and P3 undergoing positive selection following their origin from the pancereal rho and sigma duplications (Tang et al., 2010), respectively.
Divergent Expression of the Expanded SUT Groups in Monocots and Eudicots
To investigate the potential for functional diversification in the independently expanded monocot (Type IIB) and eudicot (Type I) SUT families, we examined their expression profiles by mining publicly available transcriptome data from diverse tissues of rice, Arabidopsis thaliana and soybean. In rice (Fujita et al., 2010; Kudo et al., 2013), the more ancestral Type II OsSUT4 (Os02g58080) and Type III OsSUT2 (Os12g44380) showed universal expression in all tissues analyzed (Figure 5A). Among the Type IIB SUTs, transcript levels of the founding member OsSUT1 (Os03g07480, clade P1) were highest in vegetative tissues, especially in stems. This is consistent with previous reports of OsSUT1 localization to phloem companion cells and sieve elements, and with its proposed functions in phloem loading and in carbohydrate storage and remobilization (Scofield et al., 2002, 2007a,b). OsSUT1 transcripts were also present in reproductive tissues, but at lower levels. In contrast, transcripts of the positively selected members OsSUT3 (Os10g26470, clade P2) and OsSUT5 (Os02g36700, clade P3) were only detected in reproductive tissues, with spatiotemporal specificities (Figure 5A). During pollen development, OsSUT5 transcripts were most abundant in uninucleate microspores, but declined sharply in subsequent (bi- and tri-cellular) stages. A reverse pattern was observed for OsSUT3, with highest levels found in tri-cellular pollen grains (Figure 5A). High levels of OsSUT5 transcripts were also detected in ovary and stigma during fertilization and embryogenesis (Figure 5A). Similar spatiotemporal expression patterns were observed in indica rice (Wang et al., 2010; Peng et al., 2012) (data not shown). The complementary expression patterns of clades P2 and P3 SUTs in reproductive tissues are consistent with subfunctionalization following their divergence from clade P1 by positive selection in monocots.
Figure 5. Heatmap illustration of SUT gene expression profiles across vegetative and reproductive tissues. (A) Rice SUT expression profiles. (B) Arabidopsis SUT gene expression profiles. (C) soybean SUT gene expression profiles. The scale bar depicts the relative expression strength (red, high expression; blue, low expression). SUT group and subclade designation are shown at the bottom. Tissue codes shown in parentheses for (A,B) are from the original data sources (see Materials and Methods).
In Arabidopsis thaliana, the Type I founding member AtSUC2 (At1g22710, clade B1), known to function in phloem loading (Truernit and Sauer, 1995; Gottwald et al., 2000), exhibited the highest SUT transcript levels in most of the tissues examined (Figure 5B). AtSUC1 (At1g71880) from clade B2 showed complementary expression, especially in roots and pollen where AtSUC2 transcript levels were low. However, AtSUC1 can complement the growth defects of atsuc2 mutants when expressed from the AtSUC2 promoter (Wippel and Sauer, 2012), suggesting subfunctionalization via partitioned expression between duplicated genes. Complementary expression was also observed between B2 members, with AtSUC5 (At1g71890, tandem duplicate of AtSUC1) exhibiting an embryo-specific expression, and between B1/B2 and B3 clades, with AtSUC9 (At5g06170) transcripts detected at very high levels in germinating pollen tubes (Qin et al., 2009), followed by AtSUC8 (At2g14670) and AtSUC7 (At1g66570) (Figure 5B). AtSUC7 and AtSUC6 (At5g43610) are pseudogenes, exhibiting extensive alternative splicing (AtSUC7) or sequence substitutions (AtSUC6) that are predicted to encode aberrant proteins (Sauer et al., 2004). Together, our analysis showed that multiple rounds of duplication in the Brassicaceae gave rise to an expanded Type I subfamily, with evidence of subfunctionalization in reproductive tissues.
In soybean, the most broadly expressed SUT genes belong to Type I clades F1 (Glyma10g36200) and F2 (Glyma02g08260 and Glyma16g27350), and their transcript levels were generally higher in vegetative than reproductive tissues (Figure 5C). In contrast, two members of the expanded clade F3 (Glyma02g08250 and Glyma16g27320) were much more highly expressed in embryonic and seed tissues, complementary to the pattern of clade F2 members. Expression of the remaining two F3 members was near the detection limit (Figure 5C). Thus, similar to the findings from Arabidopsis thaliana, lineage-specific expansion of Type I SUTs in soybean was also followed by expression partitioning in reproductive tissues.
The Bayesian inference of SUT phylogeny from 41 genome-sequenced plant taxa, including six basal lineages, has uncovered a complex evolutionary history of both ancient and relatively recent origins. The presence of distinct AG1 and AG2 SUTs in moss (Event 1, Figure 6) suggests that SUT diverged very early in the ancestral bryophyte, perhaps concomitant with terrestrial colonization. Major adaptations, such as osmoregulation, desiccation tolerance, and acquisition of elaborate transport capabilities to support growth and carbon-based metabolism (Rensing et al., 2008) have all been associated with higher plant SUT functions (Sauer, 2007; Kühn and Grof, 2010; Aoki et al., 2012; Frost et al., 2012). Another major evolutionary event of ancient SUTs is the divergence of gene structure (i.e., acquisition of introns) dating back to the advent of vascular plants (Event 2, Figure 6): moss SUTs are intronless within the CDS, whereas spikemoss SUTs harbor 5 and 13 introns in AG1 and AG2, respectively, similar to modern angiosperm Type II and Type III members. Interestingly, the expanded AG1 SUTs are more divergent in spikemoss (71–79% amino acid sequence similarity with one another) than in moss (88–95% similarity). This suggests that diversification of AG1 SUT may be important for developmental innovations associated with the transition from non-vascular to vascular growth habits, namely the evolution of a dominant, vascularized and branched plant body with roots, shoots and leaves (Langdale, 2008). Variation in gene sequence and structure may be linked to functional adaptation of SUTs to cope with the increasing complexity of intra/intercellular distribution of sucrose in lycophytes. Diversification of AG1 SUTs ultimately led to distinct Type I and Type III SUTs in Amborella that share a 67% amino acid sequence similarity and the same intron loss event from the progenitor AG1 (Event 3, Figure 6). Type I SUT was subsequently lost in the monocot lineages (Event 4), perhaps concomitant with evolution of Type IIB from Type II in these taxa (Event 5, Figure 6). Lineage-specific expansion of Type I (Event 6) and Type IIB (Event 7) further shaped SUT family evolution in modern angiosperms.
Figure 6. Schematic representation of SUT family evolution in angiosperms. Major events include (1) SUT divergence into AG1 and AG2 in the ancestral bryophyte, (2) intron acquisition of AG1 and AG2, and expansion and diversification of AG1 SUTs in the progenitor vascular plant, (3) diversification of Type I and Type III SUTs in the basal angiosperm, (4) loss of Type I SUTs in the ancestral monocot, (5) origin of Type IIB from Type II in the ancestral monocot, (6) intron loss and recurring episodes of lineage-specific Type I expansion (gray triangle)in eudicot‘ (7) multiple cereal-specific duplications of Type IIB (gray triangle) yielding three subclades (P1 to P3). Modern Type II and Type III SUTs represent evolutionarily conserved descendants of ancient groups AG2 and AG1, respectively. The reference landmarks of angiosperm evolution at the bottom are not to scale.
Modern Type I and Type III SUTs are functionally distinct, with plasma membrane-localized Type I involved in apoplastic phloem loading and tonoplastic Type III modulating vacuolar sucrose efflux (Sauer, 2007; Kühn and Grof, 2010; Braun et al., 2014). It was previously proposed that Type I originated from Type III via loss of the vacuolar targeting sequence after monocots and dicots diverged (Reinders et al., 2012). While our analysis supports Type I as the derived group, its evolution from Type III predates the ancestral angiosperm (Event 3, Figure 6). Both inclusion of basal lineages and gene structure analysis were instrumental for clarifying this aspect of SUT family evolution. Diversification of Type I and Type III SUTs may be linked to evolution of phloem (i.e., ‘modern’ phloem with specialized accessory cells) to support long-distance transport of photoassimilates (van Bel, 1999). Type I SUT has contrasting fates in modern flowering plants: this group was lost in monocots (Event 4) but was significantly expanded in eudicots following an intron-loss event in the progenitor eudicot (Event 6). The presence of multiple Type I SUTs in the majority of eudicot taxa we examined, including both highly divergent (e.g., Vitis and Mimulus) and similar (e.g., Populus and Malus) paralogs (Figure 2A), suggested preferential and recurring retentions of Type I duplicates following ancient as well as recent WGDs. Indeed, lineage-specific duplication/retention is the most significant driver of Type I subfamily expansion. We observed expression partitioning of the expanded Type I SUTs in both Arabidopsis and soybean, with genes descending from the most recent duplication (i.e., clades B3 and F3, respectively) exhibiting reproductive tissue-specific expression. Thus, expansion and subfunctionalization of Type I SUT appear to be a recurring theme in some eudicot lineages, with adaptive significance in reproduction.
Like Type III of AG1, Type II represents the evolutionarily conserved subfamily in AG2, with predominately single-copy presence, conserved gene structure across monocots and eudicots, and a phylogeny largely congruent with the species tree. Type II differs from the other SUTs with an extended cytoplasmic loop and as-yet-undefined function, though they are localized to the plasma membrane (Sauer, 2007; Kühn and Grof, 2010; Braun et al., 2014). Type IIB likely arose from Type II via the monocot-specific ancient polyploidy event reported by Tang et al. (2010), followed by loss of the central cytoplasmic loop in the progenitor of commelinid monocots (Event 5, Figure 6). In a striking parallelism to eudicot Type I SUTs, Type IIB (founding clade P1) was significantly expanded in Poaceae, giving rise to clades P2 and P3 (Event 7). Both the P2 and P3 clades were under positive selection, which might have contributed to their functional specialization. As is the case with the expanded Arabidopsis and soybean Type I families, partitioned tissue expression is evident among the expanded rice Type IIB family, with duplicated members also exhibiting biased expression in reproductive tissues. These data support convergent evolution of the expanded Type I and Type IIB SUTs in multiple unrelated angiosperm taxa, whereby the more recently derived members independently acquired specialized expression in reproductive tissues.
Interestingly, functional similarity between independently evolved Type I and Type IIB SUTs has also been reported for their founding (more ancestral) members, e.g., clades B1 and P1, respectively. Several of these SUTs (e.g., Arabidopsis AtSUC2, rice OsSUT1 and maize ZmSUT1/Zm2G034302) are plasma membrane-localized and function in apoplastic phloem loading (Truernit and Sauer, 1995; Gottwald et al., 2000; Scofield et al., 2007a; Slewinski et al., 2009). Expression of the barley HvSUT1 (ortholog of OsSUT1 and ZmSUT1) successfully complemented the growth defect of the Arabidopsis atsuc2 mutant, supporting functional equivalence of Type I and Type IIB founding members (Reinders et al., 2012). Convergent evolution of phylogenetically distinct SUTs in phloem loading may be associated with independent vascular development of monocots and dicots during angiosperm evolution. Monocots and dicots differ in their vascular organization, and monocots lack vascular cambia to support secondary growth (Scarpella and Meijer, 2004). Because secondary growth predates the gymnosperm-angiosperm split, it is believed that the vascular cambium was lost in the ancestral monocot (Spicer and Groover, 2010). This is consistent with the more ancestral (pre-Amborella) origin of Type I SUT (Event 3, Figure 6), and their adaptive function in phloem loading accompanying evolution of phloem and secondary growth. The loss of the vascular cambium in monocots likely rendered Type I disposable (Event 4). Acquisition of phloem loading function by the expanded Type IIB SUT (Event 5) likely co-evolved with the highly modified vascular system of monocots. Convergent evolution of reproductive tissue-biased expression of Type I and Type IIB SUTs in distinct taxa is consistent with the dependence of reproductive sink organs on phloem-mediated long-distance transport of sucrose (Gottwald et al., 2000).
In summary, the present work expands on previous studies and identifies several key drivers of plant SUT family evolution. Marked gene structure and sequence divergence of AG1 SUT accompanied the early evolution of vascular plants, culminating in functionally distinct Type I and Type III SUT families predating basal angiosperms. The evolutionarily conserved Type II and Type III SUTs appear to be under purifying selection after recurring WGD events in angiosperm evolution, whereas Type I and Type IIB SUTs underwent differential evolution, via gene loss and/or expansion, in a lineage-specific manner. Independent episodes of convergent evolution of eudicot Type I and monocot Type IIB SUTs are linked to differential vascular development in these taxa, associated with SUT function in phloem loading and reproductive fitness of flowering plants. Our work also provides a phylogenomic basis for unifying the nomenclature of plant SUT family.
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 authors thank Scott Harding for helpful discussion and critical review of the manuscript. This work was supported by the U.S. Department of Energy, Office of Biological and Environmental Research (award no. DE-SC0005140).
The Supplementary Material for this article can be found online at: http://www.frontiersin.org/journal/10.3389/fpls.2014.00615/abstract
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Keywords: transporters, phloem, vascular evolution, angiosperms, molecular evolution, expression partitioning
Citation: Peng D, Gu X, Xue L-J, Leebens-Mack JH and Tsai C-J (2014) Bayesian phylogeny of sucrose transporters: ancient origins, differential expansion and convergent evolution in monocots and dicots. Front. Plant Sci. 5:615. doi: 10.3389/fpls.2014.00615
Received: 22 September 2014; Accepted: 20 October 2014;
Published online: 12 November 2014.
Edited by:Jon Pittman, University of Manchester, UK
Reviewed by:Johannes Liesche, University of Copenhagen, Denmark
Maryse Laloi, University of Poitiers, France
Copyright © 2014 Peng, Gu, Xue, Leebens-Mack and Tsai. 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: Chung-Jui Tsai, Warnell School of Forestry and Natural Resources, University of Georgia, 120 Green Street, Davison Life Sciences B310, Athens, GA, 30602, USA e-mail: firstname.lastname@example.org