Impact Factor 4.298

The 1st most cited journal in Plant Sciences

Original Research ARTICLE

Front. Plant Sci., 20 October 2017 | https://doi.org/10.3389/fpls.2017.01811

VvVHP1; 2 Is Transcriptionally Activated by VvMYBA1 and Promotes Anthocyanin Accumulation of Grape Berry Skins via Glucose Signal

Tianyu Sun, Lili Xu, Hong Sun, Qianyu Yue, Heng Zhai and Yuxin Yao*
  • State Key Laboratory of Crop Biology, Key Laboratory of Biology and Genetic Improvement of Horticultural Crops (Huang-Huai Region), Ministry of Agriculture, College of Horticulture Science and Engineering, Shandong Agricultural University, Tai’an, China

In this work, four vacuolar H+-PPase (VHP) genes were identified in the grape genome. Among them, VvVHP1; 2 was strongly expressed in berry skin and its expression exhibited high correlations to anthocyanin content of berry skin during berry ripening and under ABA and UVB treatments. VvVHP1; 2 was transcriptionally activated directly by VvMYBA1, and VvVHP1; 2 overexpression promoted anthocyanin accumulation in berry skins and Arabidopsis leaves; therefore, VvVHP1; 2 mediated VvMYBA1-regulated berry pigmentation. On the other hand, RNA-Seq analysis of WT and transgenic berry skins revealed that carbohydrate metabolism, flavonoid metabolism and regulation and solute carrier family expression were the most clearly altered biological processes. Further experiments elucidated that VvVHP1; 2 overexpression up-regulated the expression of the genes related to anthocyanin biosynthesis and transport via hexokinase-mediated glucose signal and thereby promoted anthocyanin accumulation in berry skins and Arabidopsis leaves. Additionally, modifications of sugar status caused by enhanced hexokinase activities likely play a key role in VvVHP1; 2-induced sugar signaling.

Introduction

There are two phylogenetically distinct H+-PPases in plant cells. Type I H+-PPases are K+ sensitive, and type II H+-PPases are K+ insensitive but extremely Ca2+ sensitive. Plant type I H+-PPases are usually located on the vacuolar membrane and are considered to be bona fide vacuolar markers (Rea et al., 1992; Maeshima, 2000); thus, they are also named vacuolar H+-PPases (VHPs). Additionally, increasing evidence indicates that VHPs are localized on the plasma membrane of phloem cells in Arabidopsis and other plant species (Khadilkar et al., 2016; Regmi et al., 2016); however, greater localization of AVP1 at the vacuolar membrane compared with the plasma membrane has been reported (Segami et al., 2014). VHP1 enzyme consists of a single 80 kDa polypeptide (Maeshima, 2000). Type II H+-PPases localize and function in the Golgi apparatus, and their total amount in tissues is very low, less than 0.2% of the type I H+-PPase (Segami et al., 2010). Therefore, type I VHPs and H+-ATPase have been predicted to be the key enzyme for vacuolar acidification.

Multiple functions of VHP1 have been reported in plants. VHP1 localizes in the tonoplast and acidifies vacuoles in plant cells through the coupling of pyrophosphate (PPi) hydrolysis and active proton transport, and its function in generating H+ motive force is comparable to vacuolar H+-ATPase (Zhen et al., 1997). VHP1 is a critical factor in the regulation of cell turgor through its effects on secondary active transport of inorganic ions, organic acids, sugars and other osmoregulation substances across the tonoplast (Gaxiola et al., 2007). It has also been reported that AVP1 localized at the plasma membrane of the sieve element-companion cell complexes functions as a synthase and that this activity is critical for the maintenance of pyrophosphate homeostasis required for phloem function (Pizzio et al., 2015); phloem-specific AVP1 knockdown and overexpression demonstrated that AVP1 increases sucrose phloem loading, transport, and unloading into sink organs in Arabidopsis (Pizzio et al., 2015; Khadilkar et al., 2016). Additionally, VHP1 is also reported to affect auxin-dependent organogenesis and morphogenesis (Li et al., 2005; Gaxiola et al., 2007), to facilitate the gluconeogenesis during early seedling development (Ferjani et al., 2011), and to improve nutrient use efficiency (Li et al., 2014). Compared with metabolism modifications caused by VHP1s, the most reported functions of VHP1s are to enhance abiotic stress tolerance and to promote plant growth. It has been demonstrated that overexpression of AVP1 and other plant VHP1 genes can increase both salt and drought tolerance in diverse systems, including tobacco (Li et al., 2014), Arabidopsis (Gaxiola et al., 2001), alfalfa (Bao et al., 2016), and apple (Yao et al., 2011). Overexpression of VHP1 improves growth in various plant species (Li et al., 2005, 2014; Lv et al., 2008), and loss-of-function mutants (fugu5s) of AVP1 in Arabidopsis thaliana have post-germinative developmental defects (Asaoka et al., 2016); VHP1 has been considered as a yield-enhancing factor (Khadilkar et al., 2016).

In grape cells, anthocyanins are synthesized at the cytosolic surface of the endoplasmic reticulum by multiple enzymes via the flavonoid pathway (Boss et al., 1996). Most of the genes encoding enzymes in the anthocyanin biosynthesis pathway have been well studied in grapevines (Kühn et al., 2013). Of those enzymes, UDP glucose:flavonoid 3-o-glucosyltransferase (UFGT), which glycosylates anthocyanidins, is critical for anthocyanin biosynthesis in grape berry skins (Boss et al., 1996; Ford et al., 1998). The expression of this gene is transcriptionally regulated by the VvMYBA1 and VvMYBA2 transcription factors, either of which can regulate the color of the grape berry, in Vitis vinifera grapes (Kobayashi et al., 2004; Walker et al., 2007). VvMYBA1 and VvMYBA2 are closely clustered in a single locus that is referred to as the berry color locus; rare mutations in the two adjacent VvMYBA genes are essential for the genesis of white grapes (Walker et al., 2007). In parallel with their biosynthesis in the cytosol, anthocyanins are rapidly transported into the vacuole for storage. To date, two major transport models have been proposed: membrane vesicle- and membrane transporter-mediated transport (Zhao and Dixon, 2010). Concerning the transporter-mediated model, ATP-binding cassette (ABC) transporters and multidrug and toxic extrusion (MATE) transporters participate in anthocyanin transport across the tonoplast (Yazaki, 2005; Francisco et al., 2013). ABCC1, an ABC transporter, mediates the transport of glucosylated anthocyanidins, which is dependent on GSH (tripeptide glutathione) without the formation of an anthocyanin-GSH conjugate in grapevine (Francisco et al., 2013). Two grapevine MATEs, AM1 and AM3, mediate the specific transport of acylated anthocyanins in the presence of MgATP (Gomez et al., 2009).

To date, the role of VHP genes in regulating fruit pigmentation and the mechanism involved remains unknown. In this study, the grape VvVHP isoform genes were identified at the whole genome level, and their associations with berry pigmentation were evaluated. Additionally, the function of VvVHP1; 2 in promoting pigmentation was identified by its overexpression in berry skins and Arabidopsis leaves. Moreover, the mechanism underlying the regulation of VvVHP1; 2 on pigmentation was explored by investigating the interaction of VvMYBA1 and VvVHP1; 2 as well as VvVHP1; 2-induced glucose signal.

Materials and Methods

Plant Materials, Culture Conditions and Treatments

Grape berries were collected at different days after veraison (DAV) from 5-year-old ‘Kyoho’ grapevines (V. vinifera × labrusca). All berries were collected from the middle position of the clusters. Freshly separated skins were frozen in liquid nitrogen immediately and stored at -70°C for further determinations. Grape berries collected at -15 DAV were used for the ABA and UVB treatments. For ABA treatment, the berries were soaked in distilled water (control) or 100-μM ABA with a 14/10-h (light/dark) photoperiod at approximately 260 μmol m-2 s-1 at 25°C for 10 days. For UVB treatments, the spike-stalks of detached grape clusters were soaked in water and berries were continuously exposed to UVB (320 nm) generated by a UVB-emitting diode panel for 156 h. The berry skins were separated at different treatment time points and treated as described above. Berry skins were separated from the sterilized berries at veraison were in vitro cultured on MS medium supplemented with 10 mM mannoheptulose, a specific inhibitor of hexokinase (HXK), or mannitol as an osmotic control to evaluate the effects of the inhibition of HXK on gene expression.

Tobacco (Nicotiana benthamiana) plants were used for transactivation assays. Tobacco plants were grown in a tissue culture chamber at 25°C under a 16-h light (approximately 260 μmol m-2 s-1) regime daily for 60 days until transient transformation. WT and transgenic Arabidopsis seedlings grown on organic growth media were watered with 10 mM mannoheptulose or mannitol at 3-day intervals, and 3-week-old leaves were sampled to determine anthocyanin and gene expression.

Identifications and Sequence Analysis of VvVHP Gene Family in Grape

Taking the Arabidopsis VHP proteins encoded by AVP1 (At1g15690), AtVHP2;1 (At1g78920) and AtVHP2;2 (At1g16780) as references, protein blast analysis against grape genomic data1 were performed. Sequence alignments of different VHPs were performed using DNAman software (V8.0). An unrooted phylogenetic tree was generated with the neighbor-joining method using DNAman software (V8.0). Motif analysis was performed online2.

Genetic Transformation of VvVHP1; 2 and Its Promoter into Arabidopsis

The ORF of VvVHP1; 2 and its promoter PV HP1;2 were isolated using the primer pairs VHP-O1 and VHP-P1, respectively (Supplementary Table S1). For Arabidopsis transformation, the vectors of 35S:VvVHP1; 2 and PV HP1;2-GUS were constructed and the corresponding plasmids were transferred into Columbia-0 by a floral dip method mediated with Agrobacterium strain GV3101 (Clough and Bent, 1998).

Binding Assay Using a Yeast One-Hybrid System

A protein binding experiment was performed using the MatchmakerTM Gold Yeast One-Hybrid Library Screening System (Clontech, Mountain View, CA, United States). Three tandem copies of MBSII elements were synthesized and inserted into pAbAi vector. The resultant plasmid was introduced into the yeast strain Y1HGold, generating an MBSII-specific bait-reporter yeast strain. The background AbAr expression of the bait-reporter strain was tested. The ORF of VvMYBA1 was amplified using the primer pair of MYB-ORF1 (Supplementary Table S1) and fused in-frame with the GAL4 activation domain of the one-hybrid vector pGADT7, generating pGAD-MYBA1. The MBSII-specific bait-reporter strain was transformed with pGADT7 or pGAD-MYBA1 plasmid, and a mutant MBSII (mMBSII) was used as a negative control. The detailed yeast one-hybrid procedure was performed according to the user manual of this system (Clontech, Mountain View, CA, United States).

Transactivation Assay

The synthesized tandem sequences containing MBSII and mMBSII were fused to the upstream of the 35S minimal promoter in pRI101-GUS (Takara, Dalian, China) to generate the MBSII and mMBSII mini-GUS plasmids. The promoter sequence of VvVHP1; 2, -2100 bp upstream of ATG, was cloned by the primer pair of VHP-P2 (Supplementary Table S1) and used to replace 35S promoter of pRI101-GUS, and the ORF, amplified by the primer pair VHP-O1 (Supplementary Table S1), was inserted upstream of GUS, generating the PV HP1;2::VHP1;2-GUSplasmid. The ORF of VvMYBA1 was inserted into pRI101, replacing GUS, which generated the 35S:MYBA1 plasmid. The constructed plasmids were introduced into Agrobacterium tumefaciens strain GV3101. The Agrobacterium-mediated transient transformation of tobacco leaves was performed as previously described (Yang et al., 2000). The agro-infiltrated plants were maintained in a moist chamber at 25°C for 48 h. GUS histochemical staining and fluorometric analysis were performed according to the methods of Jefferson et al. (1987). The GUS activity was calculated as nmol of 4-Methylumbelliferone (4-MU) per mg protein per minute under controlled conditions.

Construction of the Viral Vector and Their Administration to Grape Berries

The viral vector pIR was used and the vector construction and transfection were performed as described by Peretz et al. (2007). The pIR-GUS vector was used as the control vector and to evaluate whether IL-60 system worked in grape berries. To construct the VvVHP1; 2 overexpressing vector, the full ORF of VvVHP1; 2 were amplified from grape fruit cDNA using the primer pair VHP-O3 (Supplementary Table S1). The resultant PCR products were TA cloned into the plasmid pMD-18T. GUS gene in the pIR-GUS vector was replaced by the ORF of VvVHP1; 2 by digesting with BamH I and Xba I and ligating, and the resultant construct was designated pIR-VHP1;2. The pIR-GUS and pIR-VHP1;2 vectors were transformed into Escherichia coli cells. The plasmid DNA was extracted from the propagated E. coli cells under ampicillin selection. The spike-stalks of the grape clusters at -30 DAV were punctured with a hypodermic needle. A capillary tube was inserted into the resultant hole, and approximately 200 ng of DNA (in 50 μl) was pipetted into the tube until fully soaked up by the grape clusters. The injection was performed three times at 3-day intervals. The IL-60-BS vector was used as a helper plasmid.

RNA-Seq and Quantitative Real-time PCR (qRT-PCR)

Total RNAs were extracted using TRIzol reagent (Invitrogen, Carlsbad, CA, United States) and mRNAs were purified from total RNAs using poly-T oligo-attached magnetic beads. Sequencing libraries were generated using NEBNext® UltraTM RNA Library Prep Kit for Illumina® (#7530L, NEB, United States) following the manufacturer’s recommendations, and index codes were added to attribute sequences to each sample. RNA concentration of library was measured using the Qubit® 3.0 Flurometer (Life Technologies, Carlsbad, CA, United States), and insert size was assessed using the Agilent Bioanalyzer 2100 system (Agilent Technologies, Santa Clara, CA, United States). After RNA concentration of library and insert size were assessed, the clustering of the index-coded samples was performed on a cBot cluster generation system using HiSeq PE Cluster Kit v4-cBot-HS (Illumina) according to the manufacturer’s instructions. After cluster generation, the libraries were sequenced on an Illumina Hiseq 4000 platform and 150 bp paired-end reads were generated. Clean reads were assembled into transcripts using Cufflinks with the grape genome3 as a reference. Unigene expression levels were quantified using reads per fragments per kilobase of transcript per million mapped reads (RPKM). Unigenes differentially expressed between two samples were screened using false discovery rate <0.05 and absolute log2 (fold changes) ≥1 as the threshold. The three replicates for RNA-Seq were conducted for each sample. Real-time quantitative PCR was performed using SYBR Green MasterMix (SYBR Premix EX Taq TM, Dalian, China) on a BIO-RAD iQ5 (Hercules, CA, United States) instrument, and the primers were listed in Supplementary Table S1.

Enzyme Extraction and Activity Assays

Proteins of tonoplast membranes were isolated and VHP activities were determined according to our previously reported method (Yao et al., 2011). Total protein was extracted from 1 g fresh berry skins and 0.5 g Arabidopsis leaves and HXK activity was measured by an enzyme-linked assay according to the method of Schaffer and Petreikov (1997). Determinations were made in a 1 ml reaction mixture containing 30 mM Hepes-NaOH (pH 7.5), 1 mM MgCl2, 0.6 mM EDTA, 9 mM KCl, 1 mM NAD, 1 mM ATP, 1 unit of NAD-dependent glucose-6-phosphate dehydrogenase and 50 μl extracts. The reaction was initiated with 2 mM glucose. Reactions were carried out at 37°C and A340was monitored continuously, and HXK activity was calculated from the slope of the resulting curve. HXK activity was normalized to the protein content of the extracts, and the unit was expressed as the amount of enzyme required to phosphorylate 1 nmol of glucose at 37°C for 1 min.

Metabolite Assays

Glucose and fructose were extracted with 95% methanol and determined using a capillary electrophoresis system (Beckman P/ACE, Fullerton, CA, United States). The detailed extraction and determination methods were described in our previous study (Li et al., 2013). Glucose 6-phosphate (Glu 6-P) and fructose 6-phosphate (Fru 6-P) were extracted and assayed spectrophotometrically from 1 g fresh berry skins and Arabidopsis leaves according to the method previously described by Tobias et al. (1992). Relative anthocyanin levels were determined according to our previous method (Li et al., 2013). The relative value was calculated by the formula OD = A530–0.25A657, and the unit was expressed as U/g FW.

Results

Identification and Sequence Analysis of VvVHP Genes

Using Arabidopsis thaliana AtVHPs as reference sequences, 4 counterparts were found in the grape genome, i.e., VIT_09s0002g07880, VIT_11s0118g00350, VIT_14s0060g01280 and VIT_09s0054g00700, designated VvVHP1;1, VvVHP1; 2, VvVHP1;3 and VvVHP2, respectively, in light of their sequence similarity to their Arabidopsis counterparts (Figure 1A). VvVHP1; 2 and VvVHP1;3 were located in chr 11 and 14, respectively, and VvVHP1;1 and VvVHP2 were on chr 9. VvVHP1;1 shared the highest sequence similarity of 89.2% to AVP1. The three VvVHP1 proteins shared 90.1% sequence similarity and exhibited less than 71.7% similarity to VvVHP2 (Figure 1A). Additionally, a highly conserved putative pyrophosphate-binding motif, DVGADLVGKVE, was found in the four VvVHP proteins; in contrast, a putative 14-3-3 protein-binding sequence was found only in the three VvVHP1s (Figure 1B). On the other hand, promoter sequence analysis identified different cis-acting elements for the four genes, suggesting their different roles in response to stresses, hormones and light (Figure 1C).

FIGURE 1
www.frontiersin.org

FIGURE 1. Phylogenetic tree of grape and Arabidopsis VHPs (A), amino acid alignment of four VvVHPs (B), and cis-acting elements in the promoters of VvVHPs (C). In (B), regions marked in boxes indicate putative pyrophosphate-binding motif DVGADLVGKVE (box 1) and putative 14-3-3 protein-binding sequence RQFNTIP (box 2). MBSII, MYB binding site involved in flavonoid biosynthetic genes regulation; MBS, MYB binding site involved in drought-inducibility; ABRE, abscisic acid responsiveness element; ACE, light responsiveness; HSE, heat stress responsiveness; MBS, MYB binding site involved in drought-inducibility; ERE, ethylene responsive element; SARE, salicylic acid responsive element.

Expression Analysis of VvVHPs in Different Tissues

The four VvVHPs were expressed in all examined tissues including root, stem, leaf and fruit. However, their expression levels varied with tissues. VvVHP1; 2 was expressed strongly in fruit while weakly in stem. VvVHP1;3 was primarily expressed in leaf. VvVHP2 showed high expression levels in stem and leaf but low levels in fruit. In contrast, VvVHP1;1 exhibited similar expression levels in different tissues (Figure 2A). On the other hand, a 2100-bp promoter sequence of VvVHP1; 2 was obtained, and its function was verified by the expression of a GUS gene driven by this sequence in Arabidopsis. Additionally, strong GUS expression was seen in Arabidopsis root, leaf, inflorescence and silique; in contrast, GUS expression was weak in stem (Figure 2B).

FIGURE 2
www.frontiersin.org

FIGURE 2. Expression levels of VvVHPs in different grape tissues (A) and expression of GUS driven by VvVHP1; 2 promoter in transgenic Arabidopsis seedlings (B). In (B,B1), wild type Arabidopsis seedling; (B2) transgenic Arabidopsis seedling; (B3) inflorescence; (B4) silique.

Anthocyanin Accumulations and Expression Analysis of VvVHPs during Berry Ripening and Under UVB and ABA Treatments

To investigate whether there was an association between anthocyanin accumulation and expression of VvVHPs, anthocyanin content and gene expression levels were detected during berry ripening and under UVB and ABA treatments. Anthocyanin content and expression levels of VvMYBA1 and VvUFGT continued to increase with berry ripening (Figures 3A,B). Similarly, the expression of VvVHP1;3 and especially VvVHP1; 2 continuously increased with ripening; in contrast, the expression of VvVHP1;1 and VvVHP2 was not clearly altered during ripening (Figure 3C). When grape clusters were subjected to UVB treatment, it was found that UVB accelerated berry pigmentation and increased the expression of VvMYBA1 and VvUFGT (Figures 4A–C; Supplementary Figure S1A). Consistently, VvVHP1; 2 exhibited higher expression levels under UVB than under dark at all of the time points and additionally, its expression was gradually up-regulated by UVB from 84 h and reached the maximum at 156 h (Figure 4E). VvVHP1;3 was induced, to lesser extents, by UVB from 44 h (Figure 4F). The two other VvVHPs were not induced by UVB (Figure 4D, G). When the berries were treated with exogenous ABA, berry pigmentation was accelerated, and the expression of VvMYBA1 and VvUFGT was strongly induced compared to CK conditions (Figures 4H–J and Supplementary Figure S1B). Consistently, the expression of VvVHP1; 2 was continuously induced by ABA and reached the peak at 10 days (Figure 4L). The other VvVHPs responded to ABA treatment in different manners, all of which were not consistent with the changing pattern of anthocyanins (Figures 4K,M,N). Therefore, the high associations of VvVHP1; 2 expression with the expression of VvUFGT and VvMYBA1 as well as with anthocyanin accumulation were found under normal, UVB and ABA conditions, suggesting the positive role of VvVHP1; 2 in regulating anthocyanin accumulation.

FIGURE 3
www.frontiersin.org

FIGURE 3. Anthocyanin content (A) and expression of VvMYBA1, VvUFGT (B) and VvVHPs (C) during berry ripening of ‘Kyoho’ grape. Values represent the means ± SD of 3 replicates.

FIGURE 4
www.frontiersin.org

FIGURE 4. Anthocyanin accumulation in the berry skins of the ‘Kyoho’ grape (A,H) and the expression of VvMYBA1 (B,I), VvUFGT (C,J), and VvVHPs (D–G,K–N) following the treatments with UVB and 100 μM ABA. RE, relative expression. Values represent the means ± SD of 3 replicates.

VvVHP1; 2 Is Transcriptionally Activated Directly by VvMYBA1

The MBSII element in the promoter of VvVHP1; 2 and the high correlation between VvVHP1; 2 and VvMYBA1 expression suggested that VvVHP1; 2 transcription is likely to be activated by VvMYBA1. To verify this hypothesis, a yeast one-hybrid assay was performed to determine whether the VvMYBA1 protein was able to bind DNA. Three tandem repeats of MBSII binding sites or mutant MBSII binding sites were inserted into the pAbAi vector (Figure 5A), which harbors the AbAr (aureobasidinr) reporter gene, and the corresponding constructs were designated pAbAi-MBSII and pAbAi-mMBSII. The two constructs were integrated into the genome of the yeast strain Y1HGold. AbAr basal expression assays showed that 500 ng.ml-1 AbA could completely suppress the basal expression of pAbAi-MBSII reporter strain in the absence of prey. The full-length coding sequence of VvMYBA1 was subsequently cloned into the yeast expression vector pGADT7, which harbors the GAL4 activation domain. The resulting pGADT7-MYBA1 and pGADT7 constructs were transformed into the yeast strain Y1HGold carrying the pAbAi-MBSII or pAbAi-mMBSII plasmids. All of the transformed yeast cells grew on leucine (Leu) and uracil (Ura), confirming the success of transformation (Figure 5B). As expected, only the yeast clones with pAbAi-MBSII and pGADT7-MYBA1 grew on SD/-Leu medium containing 500 ng. ml-1 AbA, suggesting that VvMYBA1 bound to the MBSII element and activated transcription in this yeast system.

FIGURE 5
www.frontiersin.org

FIGURE 5. Characterization of transcription activation of VvVHP1; 2 by VvMYBA1. (A) The sequence of the triple tandem repeats of MBSII and mMBSII binding elements. (B) Yeast one-hybrid assay using the 3 × MBSII and mMBSII as bait. Yeast cells carrying pGAD-MYBA1 or pGAD were grown on SD/-Leu/-Ura or SD/-Leu containing 500 ng.ml-1 AbA. (1) pAbAi-MBSII/pGAD-MYBA1; (2) pAbAi-MBSII/pGAD7; (3) pAbAi-mMBSII/pGAD-MYBA1; (4) pAbAi-mMBSII/pGAD7. (C,D) Histochemical analysis of the transactivation activity of VvMYBA1 via binding MBSII element. Round slices from 9-week-old tobacco leaves were agro-infiltrated with MBSII-35S mini-GUS alone (C1), with mMBSII-35S mini-GUS and 35S::MYBA1 (C2), with MBSII-35S mini-GUS and 35S::MYBA1 (C3), with PV HP1;2::VHP1;2-GUS (D1), and with PV HP1;2::VHP1;2-GUS and 35S:MYBA1. GUS staining was performed 2 days after the transformation. (E) GUS activities of the tobacco leaves infiltrated by agrobacterium containing different constructs. (F) VvVHP1; 2 expression in the tobacco leaves infiltrated by agrobacterium containing D2 and D2 constructs (D1 and D2 were denoted in D).

To investigate whether VvMYBA1 activated gene expression by interacting with the MBSII element in plant cells, Agrobacterium-mediated transient expression of a GUS reporter gene in tobacco leaves was performed. The leaves co-transformed with MBSII-35S mini-GUS and 35S:MYBA1 had bluer color and higher GUS activity than those leaves transformed with mMBSII-35S mini-GUS and 35S:MYBA1 or only MBSII-35S mini-GUS (Figures 5C,E), indicating that the GUS reporter gene was activated in tobacco leaves due to the interaction between MYBA1 and the MBSII element. Additionally, the tobacco leaves co-transformed with PV HP1;2::VHP1;2-GUS (VHP1;2-GUS fusion gene driven by VvVHP1; 2 promoter) and 35S:MYBA1 and those transformed with only PV HP1;2::VHP1;2-GUS were obtained. The results showed that the transcripts of VvVHP1; 2 and GUS activity were positively regulated by VvMYBA1 (Figures 5D–F). Therefore, VvMYBA1 acts up-stream of VHP1;2 to activate its transcript levels.

Overexpression of VvVHP1; 2 Positively Contributes to Anthocyanin Accumulation

To elucidate whether VvVHP1; 2 could promote berry pigmentation, a viral transient expression system was employed to overexpress VvVHP1; 2. When IL-60-BS and pIR-GUS were co-administered to the grape berries, GUS activity was detected by staining in the berry skins and pulps (Figure 6A), indicating that the vector system worked in grape berries under the applied conditions. The transfection of pIR-VHP1;2 clearly promoted skin pigmentation and anthocyanin accumulation in the berry skins at the two sampling time points concomitantly with the enhanced VvVHP1; 2 expression and total vacuolar PPase activities (Figures 6B–E). On the other hand, VvVHP1; 2 was introduced into Arabidopsis to evaluate its ex planta functions. qRT-PCR with primers specific to VvVHP1; 2 detected different levels of VvVHP1; 2 transcripts in the leaves of two selected transgenic lines, while no VvVHP1; 2 was detectable in the WT plants (Figure 6F), indicating that VvVHP1; 2 was ectopically expressed in these transgenic Arabidopsis lines. Additionally, the leaves of the transgenic lines exhibited strong pigmentation and high content of anthocyanins compared to the WT controls (Figures 6G,H). Therefore, overexpression of VvVHP1; 2 increased endogenous transcripts of VvVHP1; 2 and VHP activities and thereby promoted anthocyanin accumulation.

FIGURE 6
www.frontiersin.org

FIGURE 6. Overexpression of VvVHP1; 2 promoted anthocyanin accumulations in transgenic berry skins (A–E) and Arabidopsis leaves (F–H). (A) Histochemical GUS staining of pIR-GUS transfected berry skins and pulps. (B–E) Pigmentation at 0 DAV, gene expression, enzyme activity and anthocyanin content in berry skins at 0 and 16 DAV; the grape berries were transfected three times from –30 DAV at 3-day interval. (F–H) The expression, anthocyanin content and pigmentation in the 3-week-old WT and transgenic Arabidopsis leaves. The Arabidopsis seedlings were treated with 10-mM mannoheptulose or mannitol as an osmotic control from germination at 3-day intervals. Manno represents mannoheptulose.

VvVHP1; 2 Overexpression Promotes Anthocyanin Biosynthesis and Transport via Glucose Signal

To explore the mechanism underlying the regulation of VvVHP1; 2 on pigmentation, RNA-Seq analysis of the WT and transgenic berry skins was performed to quantify gene changes. It was found that 354 and 409 genes were up- and down-regulated, respectively, in the transgenic skins (Supplementary Table S2). All of the annotated DGE genes were associated with 12 biological processes. The processes of carbohydrate metabolism, flavonoid metabolism and regulation, solute carrier family, amino acid metabolism and plant hormone signal transduction were clearly changed (Figure 7A). The processes of carbohydrate metabolism contained the most DGE genes, which are associated with glycolysis/gluconeogenesis, pentose and glucoronate interconversions, starch and sucrose metabolism, and so on (Supplementary Table S2), indicating the wide modification of carbohydrate metabolism by VvVHP1; 2 overexpression. Particularly, the expression of HXK1, trehalose-phosphate phosphatase (TPP) and sucrose-phosphate synthase, which are involved in sugar signaling, were significantly up-regulated (Supplementary Table S2). A total of 32 genes involved in flavonoid metabolism and regulation were up-regulated, including anthocyanidin 3-O-glucosyltransferase 5, anthocyanidin 5,3-O-glucosyltransferase, UFGT, MYBA1 and MYBA2 (Supplementary Table S2). The solute carrier family contained 31 DGE genes, including bidirectional sugar transporter SWEET15 and SWEET 14, sucrose transporter 1 (SUT1), glucose-6-phosphate translocator 2, and anthocyanin multidrug and toxic efflux transporter (MATE) 3 and 6 (Supplementary Table S2). Moreover, the expression levels of seven genes related to sugar signaling and anthocyanin biosynthesis and transport were detected by qRT-PCR, which validated that all of the detected genes were up-regulated to varying extents (Figure 7B), consistent with the RNA-Seq results. Therefore, pathways related to sugar signaling as well as anthocyanin biosynthesis and transport were altered by VvVHP1; 2 overexpression.

FIGURE 7
www.frontiersin.org

FIGURE 7. Biological processes of differentially expressed genes classified by gene ontology (A) and the most differentially expressed genes related to sugar signaling, anthocyanin biosynthesis and transport (B). Fold changes from qRT-PCR at 0 and 16 DAV (B) were used to validate the DGE genes and to determine the expression changes of the DGE genes at different time points. Fold change from qRT-PCR was calculated by comparing the relative expression values of the selected genes in the transgenic and WT plants. Data are presented as the means of three replicates. Accession no of the genes are as follows: VvHXK1, XM_002283572; VvTPP, XP_002263078; VvMATE3, XM_002280387; VvMYBA1, AB097923; VvUFGT, AF000372.

To further verify the regulation of glucose signaling by VvVHP1; 2, mannoheptulose, a specific inhibitor of HXK, was used to treat grape skins and Arabidopsis seedlings. The results showed that the mannoheptulose treatment reduced the VvVHP1; 2 overexpression-induced increases in the expression of VvMYBA1, VvUFGT and VvMATE3 in berry skins and AtPAP1 and AtUF3GT in Arabidopsis leaves (Figures 8A,B). Additionally, anthocyanin content of transgenic Arabidopsis leaves was largely decreased by mannoheptulose treatment (Figures 6G,H). Therefore, the mannoheptulose treatment reduced the transcriptional up-regulations of the genes related to anthocyanin biosynthesis and transport and thereby decreased anthocyanin accumulation in the VvVHP1; 2 overexpressing tissues, indicating that VvVHP1; 2 regulated pigmentation via glucose signal.

FIGURE 8
www.frontiersin.org

FIGURE 8. The expression levels of genes related to anthocyanin biosynthesis and transport (A,B), hexokinase activity (C,D) and phosphorylated and non-phosphorylated sugar content (E,F) in the WT and transgenic berry skins and Arabidopsis leaves. Gene expression was detected in the in vitro cultured berry skins on MS medium containing 10 mM mannitol, as an osmotic control (pIR-GUS and pIR-VHP1;2), and mannoheptulose (pIR-VHP1;2+ Mannoheptulose) (A), and in the leaves of Arabidopsis seedlings treated with mannoheptulose and mannitol (B). Hexokinase activity (C,D) and sugar content (E,F) were determined in the berry skins at 0 DAV and 3-week-old Arabidopsis leaves. Values represent the means ± SD of 3 replicates. significant difference; ∗∗highly significant difference. The difference was not significant at 5% significant level among the values labeled with the same letter. In (B), letters and letters in brackets correspond to the comparison of AtPAP1 and AtUF3GT, respectively; manno represents mannoheptulose. Accession no of the genes are as follows: AtPAP1, AF325123; AtUF3GT, NM_124785; the others are the same as Figure 7.

In the meantime, total HXK activity as well as content of phosphorylated and non-phosphorylated glucose and fructose was determined (Figure 8). Overexpression of VvVHP1; 2 led to significant increases of HXK activity in transgenic berry skins and Arabidopsis leaves when compared with WT controls (Figures 8C, D). The content of phosphorylated and non-phosphorylated glucose and fructose as well as their ratios were enhanced by VvVHP1; 2 overexpression to varying extents and particularly, the increases of Glu 6-P and Fru 6-P reached significant levels in the transgenic berry skins (Figure 8E). In contrast, VvVHP1; 2 overexpression reduced the content of glucose and fructose and significantly enhanced the content of Glu 6-P and Fru 6-P as well as the ratios of Glu 6-P/glucose and Fru 6-P/fructose in the transgenic Arabidopsis leaves (Figure 8F). Therefore, VvVHP1; 2 overexpression increased HXK activity and modified the hexose status, which favored the generation of a sugar signal.

Discussion

Two types of VHPs exist in plant cells. The number of VHP1 and VHP2 isoforms varies among different species. Three VvVHP1s and one VvVHP2 were identified at the whole genome level in grape (Figure 1A); in contrast, two VHP1s and one VHP2 were identified in cucumber (Kabała et al., 2014), one AtVHP1 (also called AVP1) and two AtVHP2s in Arabidopsis (Segami et al., 2010), and 13 VHPs in cotton (Zhao et al., 2016). The difference in VHP number might result from the different copying rates of the whole genome and the duplication rates of VHP in evolutionary history (Zhao et al., 2016). Amino acid sequences between type I and II VHPs share low sequence similarities in Arabidopsis (Drozdowicz et al., 2000), cotton (Zhao et al., 2016), cucumber (Kabała et al., 2014) and grape (Figure 1B); less than 36% sequence identity was shared by AVP1 and AVP2 (Drozdowicz et al., 2000). Additionally, it is well known that Arabidopsis AVP1 exists primarily in the tonoplast, while AVP2 is localized to the Golgi apparatus and the trans-Golgi network and is absent in the tonoplast (Segami et al., 2010). The differences in amino acid sequence and subcellular location suggested different biological roles of the two types of VHPs. In contrast, amino acid sequences of different VHP1s are highly conserved in grape (Figure 1A), Arabidopsis, tobacco, rice and other species (Zhao et al., 2016). However, the different expression patterns of VvVHP1;1, VvVHP1; 2, and VvVHP1;3 in roots, stems, leaves and fruits as well as under ABA and UVB treatments suggested their diverse functions. Similarly, wheat TaVP1, 2, and 3 are differentially regulated spatially and in response to dehydration and salinity stresses; particularly, TaVP3 is a seed development-specific gene in contrast to TaVP1 and 2 (Wang et al., 2009); tomato SlVP1 is constitutively expressed in almost all organs whereas the SlVP2 transcript occurs at a higher level in young leaves (Mohammed et al., 2012); and cucumber CsVHP1;1 was highly expressed in roots as well as in female flowers, while CsVHP1;2 is not a tissue- or developmental stage-specific gene (Kabała et al., 2014). Additionally, the determinations of auxin-mediated organ development shows that the function of AVP1s are likely to be allele specific (Asaoka et al., 2016). Therefore, VHPs most likely participate in different biological processes rather than possess redundant functions.

VvVHP1; 2 is suggested to be involved in mediating VvMYBA1-regulated berry pigmentation. The MYB/bHLH/WD40 complexes are thought to regulate the flavonoid pathway, and the MYB transcription factors determine the specificity of this complex and have been shown to directly bind to the structural gene promoters (Sainz et al., 1997). Microarray analyses of transgenic grapevines with altered expression of VvMYBA1 show that VvMYBA1 is a positive regulator of the later stages of anthocyanin biosynthesis including their glycosylation, methylation, acylation and transport into the vacuole (Rinaldo et al., 2015), and the expression of vacuolar pyrophosphatase (corresponding to VvVHP1; 2 in our study) is significantly up-regulated in the VvMYBA1 overexpressing ‘Chardonnay’ grape berries compared to non-transgenic controls (Rinaldo et al., 2015), suggesting the regulation by VvMYBA1 on VvVHP1; 2. Additionally, it was verified that VvVHP1; 2 was a target gene of VvMYBA1 and could be directly activated by VvMYBA1 (Figure 5). On the other hand, it was reported that MdMYB1 binds to the promoters of two genes encoding the B subunits of vacuolar H+-ATPase to transcriptionally activate their expression, enhancing VHA activity, and thereby regulating anthocyanin and malate accumulation by directly facilitating their transport into vacuoles in apples (Hu et al., 2016). Similarly, the up-regulation of the solute transport carriers, including MATE 3 and 6 (Figure 7B and Supplementary Table S2), suggested that VvVHP1; 2 overexpression likely promote berry pigmentation via directly facilitating anthocyanin transport across the tonoplast. Therefore, VvVHP1; 2 is transcriptionally activated by VvMYBA1 and hence promotes anthocyanin accumulation possibly by directly facilitating its transport into vacuoles.

VvVHP1; 2 induced pigmentation via sugar signaling. It is remarkable that sugar-induced anthocyanin biosynthesis has been observed in many plant species. Glucose, fructose, and sucrose increased anthocyanin accumulation in an in vitro culture system of intact detached grape berries (Dai et al., 2014); sucrose is an important signal in the regulation of strawberry fruit ripening (Jia et al., 2013), and sucrose was the most effective inducer of anthocyanin biosynthesis in Arabidopsis seedlings (Solfanelli et al., 2006). HXKs are the first demonstrated intracellular glucose sensors in plants, and the functions of the HXK1 glucose sensor are likely evolutionarily conserved (Li and Sheen, 2016). In this study, the application of mannoheptulose, a specific inhibitor of HXK, indicated the role of VvVHP1; 2 in regulating berry pigmentation via glucose signal. On the other hand, sucrose is sensed by the plant directly, through the generation of hexoses and through sugar signals such as trehalose-6-phosphate (Li and Sheen, 2016), and SUT as a potential sucrose sensor plays a key role in sucrose signaling (Barker et al., 2000). The significant up-regulation in the expression of VvSUT1 and VvTPP (a key enzyme involved in trehalose-6-phosphate conversion) suggested that VvVHP1; 2 is likely to affect sucrose signaling. Additionally, a few studies demonstrated that sugar-induced anthocyanin accumulation is suggested to result from altered expression of regulatory and structural genes, including UFGT, DFR, LDOX and CHS, and massive reprogramming in signaling transduction pathways (Solfanelli et al., 2006; Dai et al., 2014). The sucrose induction of anthocyanin biosynthetic genes may be attributed to the up-regulation of positive transcription factors such as GL3, TT8 and PAP1 concurrent with the downregulation of the negative transcription factor MYBL2 (Jeong et al., 2010). Similarly, the enhanced anthocyanin in transgenic berry skin and Arabidopsis leaves (Figures 6E,G) might be attributed to the up-regulation of VvMYBA1/AtPAP1, VvUFGT/AtUF3GT and VvMATE3 induced byVvVHP1; 2 overexpression.

Sugar is a major component of fruit. Sucrose or glucose molecule is compartmentalized with its sensors/receptors in fruit tissue, cells or subcellular spaces; whether they play a regulatory role as a signal possibly depends on their change in content at action sites (i.e., at sites at which sensors/receptors exist), rather than their total content in whole fruit (Jia et al., 2013). The following pathways might be involved in VvVHP1; 2-induced changes of sugar status and generation of sugar signals. First, HXK1 plays dual roles in signaling and metabolism (Li and Sheen, 2016); the enhanced HXK activities (Figures 8C,D) led to the changes of phosphorylated and non-phosphorylated hexoses in the VvVHP1; 2 overexpressing tissues (Figures 8E,F), which might further influence other sugar signal molecules, such as trehalose 6-P with Glu 6-P as a precursor (Griffiths et al., 2016). Therefore, VvVHP1; 2 might affect sugar signal by HXK mediated changes of sugar status. Second, sugar signals originated from different sources, including active photosynthetic cells, dynamic storage reservoir, and organs for nutrient remobilization (Li and Sheen, 2016). It has been identified that VHPs overexpression can promote soluble sugar accumulation in berry skin (Figure 8E), sweet potato leaves (Fan et al., 2017) and apple callus (Yao et al., 2011). The enhanced sugar concentration in vacuoles might elicit feedback signaling in the photosynthetic source to ensure the balance of carbon flow (McCormic et al., 2009). Therefore, VvVHP1; 2 might modify sugar signals by altering the dynamic storage of sugar. Third, SUT1 (also designated SUC1) plays a critical role in sucrose phloem loading and transport as well as cellular sugar partitioning (Fan et al., 2017); loss of SUT1 function results in reduced sucrose transport, while increased SUT1 expression results in increased sucrose transport (Kühn and Grof, 2010). The expression of SUT1 was up-regulated in the VvVHP1; 2-overexpressing berry skins, IbVP1-overexpressing sweet potato (Fan et al., 2017) and AVP1-overexpressing Arabidopsis (Gaxiola et al., 2012). Therefore, VvVHP1; 2 might promote translocation of sucrose from source to sink tissues, at least partially, via up-regulation of VvSUT1, and thereby induced modifications of sugar status. Fourth, in addition to acidifying vacuoles, the hydrolysis of cytosolic PPi is another major function of AVP1/FUGU5 in plants; the Arabidopsis thaliana fugu5 mutant, defective in AVP1, contained ∼2.5-fold higher PPi and ∼50% less sucrose than the wild type, indicating that PPi hydrolysis is essential for active gluconeogenesis to sustain post-germinative growth of Arabidopsis seedlings (Ferjani et al., 2011). Therefore, it is likely that VvVHP1; 2 affects sugar signals by activating gluconeogenesis and thereby modifying sugar status.

Conclusion

Taken together, the expression of VvVHP1; 2 among the four identified VvVHPs correlated to berry skin pigmentation, and further experiments elucidated that VvVHP1; 2 overexpression promoted anthocyanin accumulation in berry skins and Arabidopsis leaves. VvVHP1; 2 was transcriptionally activated directly by VvMYBA1, and the increases in gene expression and enzyme activity of VvVHP1; 2 elicited glucose signal via modifying sugar status. The glucose signal from VvVHP1; 2 overexpression up-regulated the expression of regulatory and structure genes related to anthocyanin biosynthesis and transport and thereby promoted anthocyanin accumulation in berry skin (Figure 9).

FIGURE 9
www.frontiersin.org

FIGURE 9. A postulated model of how VvVHP1; 2 mediates the VvMYBA1-regulated berry pigmentation in grape berry skin. VvMYBA1 binds to the promoter of VvVHP1; 2 and enhances its action. The enhanced activity of VvVHP1; 2 provides more energy for sugar transport across the tonoplast and thereby changes the balance of carbon flow. The enhanced activity of VvVHP1; 2 promotes the hydrolysis of cytosolic PPi, which is essential for active gluconeogenesis (Ferjani et al., 2011). Some other unknown pathways might participate in the VvVHP1; 2 induced changes in sugar metabolism. Through these mechanisms, VvVHP1; 2 modifies sugar status and elicits glucose signal, which is sensed by HXK1. The genes related to anthocyanin biosynthesis and transport are transcriptionally up-regulated by glucose signal and thereby anthocyanin accumulation is promoted. VvMYBA1 directly transcriptionally activates the expression of VvVHP1; 2 and in turn the glucose signal elicited by VvVHP1; 2 enhanced the VvMYBA1 expression, which likely strengthens the process of the VvVHP1; 2-mediated berry skin pigmentation. Solid lines show experimentally demonstrated process, while dashed lines represent hypothetical process.

Author Contributions

YY and HZ designed and supervised the research. TS, LX, HS, and QY carried out the experiments. TS and HS performed data analysis. YY wrote the paper. All authors reviewed the manuscript.

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.

Acknowledgments

This work was supported by Natural Science Foundation of Shandong Province (ZR2015CM014), Funds of Shandong “Double Tops” Program (SYL2017YSTD10), China’s Agricultural Research System (CARS-30-ZT-06), and the Changjiang Scholars and lnnovative Research Team in University (IRT1155).

Supplementary Material

The Supplementary Material for this article can be found online at: https://www.frontiersin.org/articles/10.3389/fpls.2017.01811/full#supplementary-material

TABLE S1 | Primers used in this study.

TABLE S2 | RNA-Seq profiles of the WT and transgenic berry skins.

FIGURE S1 | Berry pigmentation at different treatment time under UVB (A) and ABA (B) treatments.

Footnotes

  1. ^http://genomes.cribi.unipd.it/grape/
  2. ^http://bioinformatics.psb.ugent.be/webtools/plantcare/html/
  3. ^http://genomes.cribi.unipd.it/grape/

References

Asaoka, M., Segami, S., Ferjani, A., and Maeshima, M. (2016). Contribution of PPi-hydrolyzing function of vacuolar H+-pyrophosphatase in vegetative growth of Arabidopsis: evidenced by expression of uncoupling mutated enzymes. Front. Plant Sci. 7:415. doi: 10.3389/fpls.2016.00415

PubMed Abstract | CrossRef Full Text | Google Scholar

Bao, A. K., Du, B. Q., Touil, L., Kang, P., Wang, Q. L., and Wang, S. M. (2016). Co-expression of tonoplast cation/H+ antiporter and H+-pyrophosphatase from xerophyte Zygophyllum xanthoxylum improves alfalfa plant growth under salinity, drought and field conditions. Plant Biotechnol. J. 14, 964–975. doi: 10.1111/pbi.12451

PubMed Abstract | CrossRef Full Text | Google Scholar

Barker, L., Kühn, C., Weise, A., Schulz, A., Gebhardt, C., Hirner, B., et al. (2000). SUT2, a putative sucrose sensor in sieve elements. Plant Cell 12, 1153–1164. doi: 10.1105/tpc.12.7.1153

PubMed Abstract | CrossRef Full Text | Google Scholar

Boss, P. K., Davies, C., and Robinson, S. P. (1996). Expression of anthocyanin biosynthesis pathway genes in red and white grapes. Plant Mol. Biol. 32, 565–569. doi: 10.1007/BF00019111

CrossRef Full Text | Google Scholar

Clough, S. J., and Bent, A. F. (1998). Floral dip: a simplified method for Agrobacterium-mediated transformation of Arabidopsis thaliana. Plant J. 16, 735–743. doi: 10.1046/j.1365-313x.1998.00343.x

PubMed Abstract | CrossRef Full Text | Google Scholar

Dai, Z. W., Meddar, M., Renaud, C., Merlin, I., Hilbert, G., Delrot, S., et al. (2014). Long-term in vitro culture of grape berries and its application to assess the effects of sugar supply on anthocyanin accumulation. J. Exp. Bot. 65, 4665–4677. doi: 10.1093/jxb/ert489

PubMed Abstract | CrossRef Full Text | Google Scholar

Drozdowicz, Y. M., Kissinger, J. C., and Rea, P. A. (2000). AVP2, a sequence-divergent, K+-insensitive H+-translocating inorganic pyrophosphatase from Arabidopsis. Plant Physiol. 123, 353–362. doi: 10.1104/pp.123.1.353

CrossRef Full Text | Google Scholar

Fan, W. J., Wang, H. X., Wu, Y. L., Yang, N., Yang, J., and Zhang, P. (2017). H+-pyrophosphatase IbVP1 promotes efficient iron use in sweet potato [Ipomoea batatas (L.) Lam.]. Plant Biotechnol. J. 15, 698–712. doi: 10.1111/pbi.12667

PubMed Abstract | CrossRef Full Text | Google Scholar

Ferjani, A., Segami, S., Horiguchi, G., Muto, Y., Maeshima, M., and Tsukaya, H. (2011). Keep an eye on PPi: the vacuolar-type H+-pyrophosphatase regulates postgerminative development in Arabidopsis. Plant Cell 23, 2895–2908. doi: 10.1105/tpc.111.085415

PubMed Abstract | CrossRef Full Text | Google Scholar

Ford, C. M., Boss, P. K., and Høj, P. B. (1998). Cloning and characterization of Vitis vinifera UDP-glucose: flavonoid 3-o-glucosyltransferase, a homologue of the enzyme encoded by the maize Bronze-1 locus that may primarily serve to glucosylate anthocyanidins in vivo. J. Biol. Chem. 273, 9224–9233. doi: 10.1074/jbc.273.15.9224

PubMed Abstract | CrossRef Full Text | Google Scholar

Francisco, R. M., Regalado, A., Ageorges, A., Bo, J., Bassin, B. B., Eisenach, C., et al. (2013). ABCC1, an ATP binding cassette protein from grape berry, transports anthocyanidin 3-O-glucosides. Plant Cell 25, 1840–1854. doi: 10.1105/tpc.112.102152

PubMed Abstract | CrossRef Full Text | Google Scholar

Gaxiola, R. A., Gaxiola, Sanchez, C. A., Paez-Valencia, J., Brian, G., et al. (2012). Genetic manipulation of a “vacuolar” H+-PPase: from salt tolerance to yield enhancement under phosphorus-deficient soils. Plant Physiol. 159, 3–11. doi: 10.1104/pp.112.195701

PubMed Abstract | CrossRef Full Text | Google Scholar

Gaxiola, R. A., Li, J., Undurraga, S., Dang, L. M., Allen, G. J., Alper, S. L., et al. (2001). Drought- and salt-tolerant plants result from overexpression of the AVP1 H+-pump. Proc. Natl. Acad. Sci. U.S.A. 98, 11444–11449. doi: 10.1073/pnas.191389398

PubMed Abstract | CrossRef Full Text | Google Scholar

Gaxiola, R. A., Palmgren, M. G., and Schumacher, K. (2007). Plant proton pumps. FEBS Lett. 581, 2204–2214. doi: 10.1016/j.febslet.2007.03.050

PubMed Abstract | CrossRef Full Text | Google Scholar

Gomez, C., Terrier, N., Torregrosa, L., Vialet, S., Fournier-Level, A., Verries, C., et al. (2009). Grapevine MATE-type proteins act as vacuolar H+-dependent acylated anthocyanin transporters. Plant Physiol. 150, 402–415. doi: 10.1104/pp.109.135624

PubMed Abstract | CrossRef Full Text | Google Scholar

Griffiths, C. A., Paul, M. J., and Foyer, C. H. (2016). Metabolite transport and associated sugar signaling systems underpinning source/sink interactions. Biochim. Biophys. Acta 1857, 1715–1752. doi: 10.1016/j.bbabio.2016.07.007

PubMed Abstract | CrossRef Full Text | Google Scholar

Hu, D. G., Sun, C. H., Ma, Q. J., You, C. X., Cheng, L. L., and Hao, Y. J. (2016). MdMYB1 regulates anthocyanin and malate accumulation by directly facilitating their transport into vacuoles in apples. Plant Physiol. 170, 1315–1330. doi: 10.1104/pp.15.01333

PubMed Abstract | CrossRef Full Text | Google Scholar

Jefferson, R. A., Kavanagh, T. A., and Bevan, M. W. (1987). GUS fusions, beta-glucuronidase as a sensitive and versatile gene fusion marker in higher plants. EMBO J. 6, 3901–3907.

PubMed Abstract | Google Scholar

Jeong, S. W., Das, P. K., Jeoung, S. C., Song, J. Y., Lee, H. K., Kim, Y. K., et al. (2010). Ethylene suppression of sugar-induced anthocyanin pigmentation in Arabidopsis thaliana. Plant Physiol. 154, 1515–1531. doi: 10.1104/pp.110.161869

PubMed Abstract | CrossRef Full Text | Google Scholar

Jia, H., Wang, Y., Sun, M., Li, B., Han, Y., Zhao, Y., et al. (2013). Sucrose functions as a signal involved in the regulation of strawberry fruit development and ripening. New Phytol. 198, 453–465. doi: 10.1111/nph.12176

PubMed Abstract | CrossRef Full Text | Google Scholar

Kabała, K., Janicka-Russak, M., Reda, M., and Migocka, M. (2014). Transcriptional regulation of the V-ATPase subunit c and V-PPase isoforms in Cucumis sativus under heavy metal stress. Physiol. Plant. 150, 32–45. doi: 10.1111/ppl.12064

PubMed Abstract | CrossRef Full Text | Google Scholar

Khadilkar, A. S., Yadav, U. P., Salazar, C., Shulaev, V., Paez-Valencia, J., Pizzio, G. A., et al. (2016). Constitutive and companion cell-specific overexpression of AVP1, encoding a proton-pumping pyrophosphatase, enhances biomass accumulation, phloem loading, and long-distance transport. Plant Physiol. 170, 401–414. doi: 10.1104/pp.15.01409

PubMed Abstract | CrossRef Full Text | Google Scholar

Kobayashi, S., Goto-Yamamoto, N., and Hirochika, H. (2004). Retrotransposon- induced mutations in grape skin color. Science 304, 982. doi: 10.1126/science.1095011

PubMed Abstract | CrossRef Full Text | Google Scholar

Kühn, C., and Grof, C. P. L. (2010). Sucrose transporters of higher plants. Curr. Opin. Plant Biol. 13, 287–297. doi: 10.1016/j.pbi.2010.02.001

PubMed Abstract | CrossRef Full Text | Google Scholar

Kühn, N., Guan, L., Dai, Z. W., Wu, B. H., Lauvergeat, V., Gomès, E., et al. (2013). Berry ripening: recently heard through the grapevine. J. Exp. Bot. 65, 4543–4559. doi: 10.1093/jxb/ert395

PubMed Abstract | CrossRef Full Text | Google Scholar

Li, J. S., Yang, H. B., Peer, W. A., Richter, G., Blakeslee, J., Bandyopadhyay, A., et al. (2005). Arabidopsis H+-PPase AVP1 regulates auxin-mediated organ development. Science 310, 121–125. doi: 10.1126/science.1115711

PubMed Abstract | CrossRef Full Text | Google Scholar

Li, L., and Sheen, J. (2016). Dynamic and diverse sugar signaling. Curr. Opin. Plant Biol. 33, 116–125. doi: 10.1016/j.pbi.2016.06.018

PubMed Abstract | CrossRef Full Text | Google Scholar

Li, X. J., Guo, C. J., Gu, J. T., Duan, W. W., Zhao, M., Ma, C. Y., et al. (2014). Overexpression of VP, a vacuolar H+-pyrophosphatase gene in wheat (Triticum aestivum L.), improves tobacco plant growth under Pi and N deprivation, high salinity, and drought. J. Exp. Bot. 65, 683–696. doi: 10.1093/jxb/ert442

PubMed Abstract | CrossRef Full Text | Google Scholar

Li, X. L., Wang, C. R., Li, X. Y., Yao, Y. X., and Hao, Y. J. (2013). Modifications of Kyoho grape berry quality under long-term NaCl treatment. Food Chem. 139, 931–937. doi: 10.1016/j.foodchem.2013.02.038

PubMed Abstract | CrossRef Full Text | Google Scholar

Lv, S., Zhang, K., Gao, Q., Lian, L., Song, Y., and Zhang, J. (2008). Overexpression of an H+-PPase gene from Thellungiella halophila in cotton enhances salt tolerance and improves growth and photosynthetic performance. Plant Cell Physiol. 49, 1150–1164. doi: 10.1093/pcp/pcn090

PubMed Abstract | CrossRef Full Text | Google Scholar

Maeshima, M. (2000). Vacuolar H+-pyrophosphatase. Biochim. Biophys. Acta 1465, 37–51. doi: 10.1016/S0005-2736(00)00130-9

CrossRef Full Text | Google Scholar

McCormic, A. J., Watt, D. A., and Cramer, M. D. (2009). Supply and demand: sink regulation of sugar accumulation in sugarcane. J. Exp. Bot. 60, 357–364. doi: 10.1093/jxb/ern310

PubMed Abstract | CrossRef Full Text | Google Scholar

Mohammed, S. A., Nishio, S., Takahashi, H., Shiratake, K., Ikeda, H., Kanahama, K., et al. (2012). Role of vacuolar H+-inorganic pyrophosphatase in tomato fruit development. J. Exp. Bot. 63, 5613–5621. doi: 10.1093/jxb/ers213

PubMed Abstract | CrossRef Full Text | Google Scholar

Peretz, Y., Mozes-Koch, R., Akad, F., Tanne, E., Czosnek, H., and Sela, I. (2007). A universal expression/silencing vector in plants. Plant Physiol. 145, 1251–1263. doi: 10.1104/pp.107.108217

PubMed Abstract | CrossRef Full Text | Google Scholar

Pizzio, G. A., Paez-Valencia, J., Khadilkar, A. S., Regmi, K., Patron-Soberano, A., Zhang, S. J., et al. (2015). Arabidopsis type I proton-pumping pyrophosphatase expresses strongly in phloem, where it is required for pyrophosphate metabolism and photosynthate partitioning. Plant Physiol. 167, 1541–1553. doi: 10.1104/pp.114.254342

PubMed Abstract | CrossRef Full Text | Google Scholar

Rea, P. A., Kim, Y., Sarafian, V., Poole, R. J., Davies, J. M., Sanders, D., et al. (1992). Vacuolar H+-translocating pyrophosphatases: a new category of ion translocase. Trends Biochem. Sci. 17, 348–353. doi: 10.1016/0968-0004(92)90313-X

CrossRef Full Text | Google Scholar

Regmi, K. C., Zhang, S., and Gaxiola, R. A. (2016). Apoplasmic loading in the rice phloem supported by the presence of sucrose synthase and plasma membrane-localized proton pyrophosphatase. Ann. Bot. 117, 257–268. doi: 10.1093/aob/mcv174

PubMed Abstract | CrossRef Full Text | Google Scholar

Rinaldo, A. R., Cavallini, E., Jia, Y., Moss, S. M. A., McDavid, D. A. J., Hooper, L. C., et al. (2015). A grapevine anthocyanin acyltransferase, transcriptionally regulated by VvMYBA, can produce most acylated anthocyanin present in grape skins. Plant Physiol. 169, 1897–1916. doi: 10.1104/pp.15.01255

PubMed Abstract | CrossRef Full Text | Google Scholar

Sainz, M. B., Grotewold, E., and Chandler, V. L. (1997). Evidence for direct activation of an anthocyanin promoter by the maize C1 protein and comparison of DNA binding by related Myb domain proteins. Plant Cell 9, 611–625. doi: 10.1105/tpc.9.4.611

PubMed Abstract | CrossRef Full Text | Google Scholar

Schaffer, A. A., and Petreikov, M. (1997). Sucrose-to-starch metabolism in tomato fruit undergoing transient starch accumulation. Plant Physiol. 113, 739–746. doi: 10.1104/pp.113.3.739

PubMed Abstract | CrossRef Full Text | Google Scholar

Segami, S., Makino, S., Miyake, A., Asaoka, M., and Maeshima, M. (2014). Dynamics of vacuoles and H+-pyrophosphatase visualized by monomeric green fluorescent protein in Arabidopsis: artifactual bulbs and native intravacuolar spherical structures. Plant Cell 26, 3416–3434. doi: 10.1105/tpc.114.127571

PubMed Abstract | CrossRef Full Text | Google Scholar

Segami, S., Nakanishi, Y., Sato, M. H., and Maeshima, M. (2010). Quantification, organ-specific accumulation and intracellular localization of type II H+-pyrophosphatase in Arabidopsis thaliana. Plant Cell Physiol. 51, 1350–1360. doi: 10.1093/pcp/pcq096

PubMed Abstract | CrossRef Full Text | Google Scholar

Solfanelli, C., Poggi, A., Loreti, E., Alpi, A., and Perata, P. (2006). Sucrose-specific induction of the anthocyanin biosynthetic pathway in Arabidopsis. Plant Physiol. 140, 637–646. doi: 10.1104/pp.105.072579

PubMed Abstract | CrossRef Full Text | Google Scholar

Tobias, R. B., Boyer, C. D., and Shannon, J. C. (1992). Alterations in carbohydrate intermediates in the endosperm of starch-deficient maize (Zea mays L.) genotypes. Plant Physiol. 99, 146–152. doi: 10.1104/pp.99.1.146

PubMed Abstract | CrossRef Full Text | Google Scholar

Walker, A. R., Lee, E., Bogs, J., McDavid, D. A. J., Thomas, M. R., and Robinson, S. P. (2007). White grapes arose through the mutation of two similar and adjacent regulatory genes. Plant J. 49, 772–785. doi: 10.1111/j.1365-313X.2006.02997.x

PubMed Abstract | CrossRef Full Text | Google Scholar

Wang, Y., Xu, H., Zhang, G., Zhu, H., Zhang, L., Zhang, Z., et al. (2009). Expression and responses to dehydration and salinity stresses of V-PPase gene members in wheat. J. Genet. Genomics 36, 711–720. doi: 10.1016/S1673-8527(08)60164-2

PubMed Abstract | CrossRef Full Text | Google Scholar

Yang, Y., Li, R., and Qi, M. (2000). In vivo analysis of plant promoters and transcription factors by agroinfiltration of tobacco leaves. Plant J. 22, 543–551. doi: 10.1046/j.1365-313x.2000.00760.x

PubMed Abstract | CrossRef Full Text | Google Scholar

Yao, Y. X., Dong, Q. L., You, C. X., Zhai, H., and Hao, Y. J. (2011). Expression analysis and functional characterization of apple MdVHP1 gene reveals its involvement in Na+, malate and soluble sugar accumulation. Plant Physiol. Biochem. 49, 1201–1208. doi: 10.1016/j.plaphy.2011.05.012

PubMed Abstract | CrossRef Full Text | Google Scholar

Yazaki, K. (2005). Transporters of secondary metabolites. Curr. Opin. Plant Biol. 8, 301–307. doi: 10.1016/j.pbi.2005.03.011

PubMed Abstract | CrossRef Full Text | Google Scholar

Zhao, J., and Dixon, R. A. (2010). The ‘ins’ and ‘outs’ of flavonoid transport. Trends Plant Sci. 15, 72–80. doi: 10.1016/j.pbi.2005.03.011

PubMed Abstract | CrossRef Full Text | Google Scholar

Zhao, X. J., Lu, X. K., Yin, Z. J., Wang, D. L., Wang, J. J., Fan, W. L., et al. (2016). Genome-wide identification and structural analysis of pyrophosphatase gene family in cotton. Crop Sci. 56, 1831–1840. doi: 10.2135/cropsci2014.12.0832

CrossRef Full Text | Google Scholar

Zhen, R. G., Kim, E. J., and Rea, P. A. (1997). The molecular and biochemical basis of pyrophosphate-energized proton translocation at the vacuolar membrane. Adv. Bot. Res. 25, 297–337. doi: 10.1016/S0065-2296(08)60156-1

CrossRef Full Text | Google Scholar

Keywords: VvVHP1; 2, VvMYA1, transcriptional regulation, anthocyanins, grape berry, glucose signal

Citation: Sun T, Xu L, Sun H, Yue Q, Zhai H and Yao Y (2017) VvVHP1; 2 Is Transcriptionally Activated by VvMYBA1 and Promotes Anthocyanin Accumulation of Grape Berry Skins via Glucose Signal. Front. Plant Sci. 8:1811. doi: 10.3389/fpls.2017.01811

Received: 20 July 2017; Accepted: 05 October 2017;
Published: 20 October 2017.

Edited by:

Claudio Bonghi, Università degli Studi di Padova, Italy

Reviewed by:

Richard Victor Espley, Plant & Food Research, New Zealand
Laura Jaakola, UiT The Arctic University of Norway, Norway

Copyright © 2017 Sun, Xu, Sun, Yue, Zhai and Yao. 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: Yuxin Yao, yaoyx@sdau.edu.cn