- Research article
- Open Access
Functional characterisation of three members of the Vitis viniferaL. carotenoid cleavage dioxygenase gene family
BMC Plant Biology volume 13, Article number: 156 (2013)
In plants, carotenoids serve as the precursors to C13-norisoprenoids, a group of apocarotenoid compounds with diverse biological functions. Enzymatic cleavage of carotenoids catalysed by members of the carotenoid cleavage dioxygenase (CCD) family has been shown to produce a number of industrially important volatile flavour and aroma apocarotenoids including β-ionone, geranylacetone, pseudoionone, α-ionone and 3-hydroxy-β-ionone in a range of plant species. Apocarotenoids contribute to the floral and fruity attributes of many wine cultivars and are thereby, at least partly, responsible for the “varietal character”. Despite their importance in grapes and wine; carotenoid cleavage activity has only been described for VvCCD1 and the mechanism(s) and regulation of carotenoid catabolism remains largely unknown.
Three grapevine-derived CCD-encoding genes have been isolated and shown to be functional with unique substrate cleavage capacities. Our results demonstrate that the VvCCD4a and VvCCD4b catalyse the cleavage of both linear and cyclic carotenoid substrates. The expression of VvCCD1, VvCCD4a and VvCCD4b was detected in leaf, flower and throughout berry development. VvCCD1 expression was constitutive, whereas VvCCD4a expression was predominant in leaves and VvCCD4b in berries. A transgenic population with a 12-fold range of VvCCD1 expression exhibited a lack of correlation between VvCCD1 expression and carotenoid substrates and/or apocarotenoid products in leaves, providing proof that the in planta function(s) of VvCCD1 in photosynthetically active tissue is distinct from the in vitro activities demonstrated. The isolation and functional characterisation of VvCCD4a and VvCCD4b identify two additional CCDs that are functional in grapevine.
Taken together, our results indicate that the three CCDs are under various levels of control that include gene expression (spatial and temporal), substrate specificity and compartmentalisation that act individually and/or co-ordinately to maintain carotenoid and volatile apocarotenoid levels in plants. Altering the expression of VvCCD1 in a transgenic grapevine population illustrated the divergence between the in vitro enzyme activity and the in planta activity of this enzyme, thereby contributing to the efforts to understand how enzymatic degradation of carotenoids involved in photosynthesis occurs. The identification and functional characterisation of VvCCD4a and VvCCD4b suggest that these enzymes are primarily responsible for catalysing the cleavage of plastidial carotenoids.
Carotenoids are hydrophobic C40 isoprenoid pigments occurring throughout the natural world. In higher plants carotenoids are typically associated with photosynthetic membranes of plastids, especially the chloroplasts where they are involved in a number of photochemical reactions. In chloroplasts carotenoids primarily act as accessory pigments in the light harvesting antennae complexes and also assist in photoprotection by quenching free radicals and preventing photo-oxidative damage to the cell. The carotenoids in chloroplasts are typically not found “free” within the aqueous stroma, but rather bound in distinct pigment-protein antenna complexes within the membranes of the thylakoids (grana) .
The localisation and composition of carotenoids change during stresses (e.g. the xanthophylls cycle), and during plastid transitions/differentiation: chloroplasts to chromoplasts (as occurs in some fruits and flowers) or chloroplasts to gerontoplasts (as occurs during senescence) . The genes and enzymes involved in carotenoid biosynthesis in plants have received much attention and the conserved pathway is relatively well characterised (reviewed in [3, 4]); similarly the genes and enzymes of the carotenoid metabolic pathway for V. vinifera have been described previously [5, 6].
The carotenoid cleavage dioxgenase (CCD) enzyme family contribute to the directed enzymatic production of apocarotenoids. Apocarotenoids and their derived metabolites have diverse biological roles (reviewed in ). In Arabidopsis thaliana nine different CCDs have been identified . Five of the Arabidopsis CCDs (NCED2, NCED3, NCED5, NCED6, and NCED9) catalyse the first step towards abscisic acid (ABA) biosynthesis . The remaining four Arabidopsis members of this protein family (CCD1, CCD4, CCD7 and CCD8) have more divergent activities and catalyse the cleavage of a variety of carotenoid substrates at specific double bond positions. Sequential cleavage catalysed by CCD7 and CCD8 are involved in formation of the shoot-branching inhibiting hormone, strigolactone . CCD1- and CCD4-catalysed cleavage results in the production of a variety of flavour and aroma compounds .
The CCD1 orthologues are highly similar and are the only members of the CCD enzyme family predicted to have a cytosolic (rather than plastidial) localisation . Orthologues have been shown to catalyse the symmetrical cleavage of a variety of carotenoids in vitro at the 5,6 (5’,6’) and 9,10 (9’,10’) double bond position producing a wide range of volatile C13-norisoprenoids. These carotenoid-derived C13-norisoprenoids are found in flowers, fruits, and leaves of many plants [12, 13] and are considered to be flavour and aroma compounds, often displaying very low detection thresholds. Due to their contribution to the fruity and floral varietal perception of wine; C13-norisoprenoids have received much interest in wine grapes ([14–16] and reviewed in ). Previous attempts to determine the role of CCD1 in plants through transgenic manipulation of its transcript levels have been performed in Solanum lycopersicum (in tomato fruit) ; Medicago truncatula (in mycorrhizal roots) ; and Oryza sativa (in rice endosperm) . These studies suggested that the observed in vitro functioning of CCD1 (i.e. catalysis of the symmetrical 9,10 (9’,10’) oxidative cleavage of carotenoids) may not be its sole biological action in planta and that other genes may code for enzyme(s) which are primarily responsible for catalysing this cleavage reaction in plastids .
To date CCD4 orthologues have only been identified in Angiosperms (flowering plants) and characterisation of CCD4 enzyme activity has shown that these members of the CCD family contribute to the carotenoid-derived flavour and aroma profile of both fruits and flowers. Subcellular localisation studies in A. thaliana and Crocus sativus (saffron)  have demonstrated that the enzymes are targeted specifically to the plastoglobules within the plastids. Unlike the cytosolic localisation of the CCD1 orthologues; the CCD4 localisation gives it access to its carotenoid substrates . CCD4 enzymes often occur as two isoforms: CCD4a and CCD4b that share modest similarity to each other and have distinct expression patterns and potentially divergent functions in plants. Based on reports from various plants there seems to be no consensus on the specific enzyme activity of the CCD4 enzymes.
Although CCD1 and CCD4 enzymes catalyse the cleavage of carotenoids at the same double bond positions; CCD4 enzymes are proposed to be substrate-specific, whereas the CCD1 enzymes are commonly described and demonstrated as more promiscuous in their substrate preferences . A study by Huang et al. concluded that CCD4s cannot catalyse the cleavage of linear carotenoids (e.g. lycopene and cis-ξ-carotene), or carotenoids that contain hydroxyl groups (e.g. zeaxanthin and lutein) and the current hypothesis is therefore that CCD4 orthologues catalyse cyclic non-polar carotenoid cleavage (e.g. β-carotene).
By identifying, isolating and characterising the grapevine CCDs, putatively involved in flavour and aroma related apocarotenoid production, the current work aimed to elucidate the biological role of these genes and their respective enzymes in grapevine. This study reports the isolation of CCD1, CCD4a and CCD4b-encoding genes from Vitis vinifera L. cv Pinotage. The CCDs were characterised by determining their expression patterns and functionality in grapevine. Functionality was described by analysing the volatile apocarotenoids formed following carotenoid cleavage in a heterologous Escherichia coli (bacterial) system. Furthermore, a population of transgenic grapevine (V. vinifera L. cv. Sultana) with altered expression of VvCCD1 (up-regulated and down-regulated) was generated and characterised genetically and phenotypically. Leaf tissue of the transgenic Sultana lines was analysed via HPLC and GC/MS for the detection and quantification of carotenoids and volatile apocarotenoids, respectively.
The National Center for Biotechnology Information (NCBI) Entrez search and retrieval system was used to obtain nucleotide and protein sequences from the Genbank databases (http://www.ncbi.nlm.nih.gov/gquery). Alignments to sequences in the Genbank databases were performed using the relevant Blast algorithm (http://www.ncbi.nlm.nih.gov/BLAST/) . Comparative genomics (i.e. gene structure prediction and homologue/orthologue retrieval) were performed via PLAZA (http://bioinformatics.psb.ugent.be/plaza/) .
The putative sub-cellular localisation of protein sequences were predicted using ProtComp Version 8.0 (http://www.softberry.com/berry.phtml). V. vinifera expressed sequence tags (ESTs) were retrieved from The Institute for Genomic Research (TIGR) Grape Gene Index (http://compbio.dfci.harvard.edu/tgi/) or NCBI. The V. vinifera genomic sequences were retrieved from NCBI or Genoscope (http://www.cns.fr/externe/GenomeBrowser/Vitis/). Protein alignments were performed with Clustal Omega (http://www.ebi.ac.uk/tools/msa/clustalo/), and the resultant phylogenetic trees visualised using MEGA .
Grapevine material for gene isolation, native expression analysis and pigment analysis was harvested from field-grown Vitis vinifera L. cv. Pinotage at Welgevallen experimental farm (Stellenbosch, South Africa). Green, véraison and ripe berries, as well as fully expanded leaf and mature flower material were harvested and flash frozen in the field in liquid nitrogen. The frozen tissue was homogenised in liquid nitrogen and, if not used immediately, stored at -80°C.
Transgenic plants were housed in a greenhouse and grown in a commercial soil mixture supplemented with Nitrosol® every 3 weeks. Analyses of gene expression, pigment concentrations and volatile composition were performed on tissue from fully expanded leaf tissue (leaf position 3 and 4). Leaves were flash frozen in liquid nitrogen immediately upon harvesting and stored in the dark at -80°C. Control plants underwent the same tissue culture, hardening-off and glass house conditions and procedures as the transgenic population.
Isolation, extraction and manipulations of nucleic acids
High molecular weight genomic DNA was isolated from fully expanded V. vinifera leaves as described by Steenkamp et al.. Total RNA from different grapevine leaves was extracted according to the methods described by Reid et al.. Unless otherwise stated, all standard methods for plasmid DNA isolation, manipulations and cloning of DNA fragments, and agarose gel electrophoresis were used as described by Sambrook et al..
Total cDNA was synthesised from 1 μg DNase I-treated (Promega, Madison, WI) total RNA using the Superscript III Platinum first strand synthesis system (Invitrogen) in a 20 μL reaction volume as described by the supplier.
Bacterial strains, media, growth conditions, and transformations
Escherichia coli (DH5α and TOP10F) and Agrobacterium tumefaciens (EHA105) cultures were grown in LB media (1.2% (w/v) tryptone, 1.2% (w/v) NaCl and 0.6% (w/v) yeast extract). Bacterial transformations were performed using the heat-shock method as described in Sambrook et al.. Transformants were selected using the appropriate antibiotic as selection on LB plates. Putative positive colonies were cultured and their plasmids isolated and verified by restriction digest. Unless otherwise stated all E. coli cultures were grown at 37°C and A. tumefaciens cultures at 30°C.
Plasmids, cloning and bacterial transformations
The carotenoid accumulating strains used to perform the functional complementation assays were obtained from F. X. Cunningham (Department of Cell Biology and Molecular Genetics, University of Maryland, MD, USA) and are described in Cunningham  and Cunningham et al.[32, 33].
The primer pair VvCCD1_5’ and VvCCD1_3’ was used to amplify the VvCCD1 gene from V. vinifera L. cv. Pinotage cDNA (Additional file 1). The primer pairs VvCCD4a_5’, VvCCD4a_3’ and VvCCD4b_5’, VvCCD4b_3’ were used to amplify VvCCD4a and VvCCD4b from V. vinifera L. cv. Pinotage cDNA (Additional file 1). The resultant PCR amplicons were cloned into the pGEM-T Easy vector system according to the specifications of the supplier (Promega), to generate the plasmids pGEMt-VvCCD1, pGEMt-VvCCD4a and pGEMt-VvCCD4b (Additional file 2).
For the construction of plasmids for bacterial functional complementation, the 1715 bp VvCCD1 coding region was excised from pGEMt-VvCCD1 as an Ndel/PstI fragment and cloned into the corresponding sites of pTWIN1 to yield pTWIN1-VvCCD1. The 1722 bp VvCCD4a coding region was excised from pGEMt-VvCCD4a as Ndel/BglII fragment and cloned into the compatible Ndel/BamHI sites of pTWIN1 to yield pTWIN1-VvCCD4a. The 1770 bp VvCCD4b coding region was excised from pGEMt-VvCCD4b as an Ndel/BamHI fragment and cloned into the corresponding sites of pTWIN1 to yield pTWIN1-VvCCD4b (Additional file 2).
The binary vector, pART27 was used for both the overexpression and silencing constructs . The 1715 bp VvCCD1 coding region was excised from pGEMt-VvCCD1 as a SalI/SpeI fragment and cloned into the compatible XhoI/XbaI sites of pART7 to yield pART7-VvCCD1. The expression cassette was excised with NotI and cloned into the corresponding site of pART27 to yield pART27-VvCCD1.
The pHANNIBAL vector was used for the construction of a VvCCD1 RNAi/silencing vector . A 148 bp fragment was PCR-amplified from the 3’ untranslated region (UTR) of VvCCD1 from V. vinifera L. cv Pinotage genomic DNA using the primer pair VvCCD1_RNAi_5’ and VvCCD1_RNAi_3’ (Additional file 1). The pGEM®-T Easy vector system was used to clone the PCR amplicon according to the specifications of the supplier (Promega), creating the pGEMt-CCD1(RNAi) plasmid. A 136 bp XhoI and EcoRI fragment was excised from pGEMt-CCD1(RNAi) and ligated into the corresponding XhoI and EcoRI sites in pHANNIBAL. The resultant plasmid was subsequently digested with BamHI and XbaI and the 148 bp BamHI and XbaI fragment from pGEMt-CCD1(RNAi) was ligated into the corresponding sites. The resultant plasmid, pHANNIBAL-CCD1(RNAi), contained a 148 bp inverted repeat of the 3’-UTR of VvCCD1. The expression cassette was excised from pHANNIBAL-CCD1(RNAi) with NotI, and ligated into the corresponding NotI site of pART27 yielding the final VvCCD1 silencing vector, pART27-CCD1(RNAi) (Additional file 2).
Grapevine transformation and regeneration
Somatic embryogenic cultures of V. vinifera L. cv. Sultana were used as source material for the genetic transformation experiments. The somatic embryogenic cultures were obtained and maintained according to the methods described in Vasanth and Vivier . The genetic transformation protocol was essentially according to Franks et al. with some modifications to use liquid cultures as starting material (as described in Vasanth and Vivier ). Briefly, Agrobacterium tumefaciens cells, containing either the overexpression or silencing vector, were harvested by centrifugation at 5,000 rpm for 10 min and resuspended in liquid NN medium, containing 18.5 μg.mL-1 maltose to a final OD600 of 0.8. Acetosyringone (19.7 mg.L-1) was added to the agrobacterial suspension before 2 mL of the somatic embryogenic cell suspensions were added and left for 15 min, with gentle shaking three to five times during this period. The culture was filtered to remove the excess liquid and the callus blotted dry using sterile Whatman no.1 filter paper. Co-cultivation proceeded at 27°C in the dark for 2 days on solid NN medium supplemented with BAP (0.25 μg.mL-1), NOA (1.0 μg.mL-1) and acetosyringone (19.7 μg.mL-1). Subsequently embryos were washed with sterile NN medium containing carbenicillin (200 μg.mL-1), blotted dry on sterilised filter paper and handled according to the protocol of Franks et al. . Selection on kanamycin (100 μg.mL-1) was maintained until in vitro rooted plantlets were obtained, and subsequently hardened off in a greenhouse.
Southern blot analysis
Southern blot analysis was performed using 10–20 μg of genomic DNA extracted from grapevine leaves. The DNA was digested with SpeI, separated in a 0.8% (w/v) TBE agarose gel and transferred to a positively charged Hybond-N nylon membrane as described by the supplier (Amersham-Pharmacia Biotech, Buckinghamshire, UK). Probe labelling, hybridisation, and Biotin detection were performed using the Biotin non-radioactive nucleic acid labelling and detection system according to the specifications of the supplier (Roche Diagnostics, Mannheim, Germany).
Expression analysis of VvCCDs
Primers for qRT-PCR for the expression analysis of VvCCD1, VvCCD4a, VvCCD4b, VvCCD4c, VvCCD4d, VvCCD7 and VvCCD8 were designed using Primer Express 3.0 (Applied Biosystems) (Additional file 1). The V. vinifera elongation factor 1α (VvEF1α) was selected as a “house-keeping” gene to normalise gene expression based on the findings of Reid et al. and Guillaumie et al.; Relative expression analysis of the VvCCD gene family was performed in three different berry developmental stages, corresponding to green, vérasion and ripe berry stages of V. vinifera L. cv Pinotage.
Expression analysis of VvCCD1 in the transgenic grapevine population was similarly performed via qRT-PCR. The grapevine glyceraldehyde-3-phosphate dehydrogenase (VvGAPDH) gene was used as a “house-keeping” gene to normalise gene expression. The expression of VvGAPDH has been shown to be relatively invariant in grapevine berries . Primers were designed to evaluate total VvCCD1 expression (i.e. endogenous and transgene-derived expression), as well as expression derived from only the transgenic VvCCD1 (Additional file 1).
Real-time PCR was performed using an Applied Biosystems 7500 Real-time PCR System. KAPA SYBR® FAST qRT-PCR Kit was used according to the manufacturer’s (Kapa Biosystems, Cape Town, South Africa) instructions. The programme for the PCR reactions was: 50°C for 2 minutes; 95°C for 10 minutes; and 40 cycles of 15 seconds at 95°C and 60 seconds at 58°C. Data were analysed using the Applied Biosystems SDS software (version 1.4). All PCR reactions consisted of at least three technical replicates. Relative expression was calculated using the equation as described by Pfaffl :
(where E is the PCR efficiency and CP is the cycle number that the florescence crosses the base line).
Bacterial functional complementation and determination of volatile apocarotenoids in bacterial headspace
The extraction and analysis of the volatile apocarotenoids from bacterial cultures were performed based on a method described in Lücker et al.. For clarity the method and relevant modifications are described in detail. pTWIN1-VvCCD1, pTWIN1-VvCCD4a and pTWIN1-VvCCD4b plasmids were introduced into carotenoid accumulating E. coli strains. An empty vector, pTWIN1, was used as a negative control. An overnight culture (5 mL) grown in LB media to saturation was used to inoculate 32 mL of LB containing the appropriate antibiotics (100 μg.mL-1 ampicillin, 34 μg.mL-1 chloroamphenicol and 12.5 μg.mL-1 tetracycline) until an OD600nm of 0.1 was reached. The cultures were incubated in the dark, gently shaking at room temperature until an OD600 nm of 0.6 was reached. To prevent further production of coloured carotenoids the inhibitor diphenylamine (DPA) was added to a final concentration of 100 μM (as described in Cunningham and Gantt ) and the cultures were incubated at room temperature for an additional two hours in the dark. After the two hour incubation with the inhibitor, 8 mL of the 32 mL culture was removed and flash frozen for carotenoid analysis; and the remaining 24 mL of culture was harvested for apocarotenoid analysis. For apocarotenoid analysis the cells were resuspended in 6 mL of LB containing the appropriate antibiotics, 0.1 mM isopropyl-β-D-thiogalactopyranoside (IPTG), and 1 ppm of α-terpineol (as internal standard, IS). In addition 6 mM ascorbate, 5 μM ferrous sulphate, 200 U/mL catalase were added as described in Baldermann et al. for in vitro CCD1 enzyme assays. The cultures were subsequently transferred to 20 ml SPME vials. The vials were sealed with Bi-metal®crimp seals with 20 mm silicone/polytetrafluoroethylene (PTFE) septa (Brown Chromatographic supplies, Wertheim, Germany). The samples were incubated in the dark, gently shaking at room temperature for 16 hours. After 16 hours, 1 mL of culture was removed for OD600nm determination and 5 mL of 5 M NaCl was added to the 5 mL remaining culture for volatile apocarotenoid extraction.
The HS-SPME extraction of volatile apocarotenoids from the bacterial cultures was performed using a CTC CombiPal auto sampler equipped with the SPME option (CTC Analytics, Switzerland). Extraction conditions were as follows: after incubation at 50°C for 2 minutes SPME extraction was performed for 15 min under constant agitation by exposing a divinylbenzene/Carboxen/polydimethylsiloxane (DVB/CAR/PDMS) SPME fibre (Supelco, Bellefonte, PA) to the headspace. Thereafter the fibre was desorbed and analytes subsequently injected onto the GC column using a split/splitless injector, operated at 240°C, splitless for 2 minutes. The fibre was left in the injector for a further 20 minutes at 270°C for conditioning of the fibre under a purge flow of 60 mL/min. Separation of compounds was achieved on a DB-FFAP column (60 m × 0.25 mm × 0.5 μm) on an Agilent 6890 gas chromatograph coupled to an Agilent 5975C mass spectrometer (MS) (Agilent Technologies, Little Falls, Wilmington, USA). The helium carrier gas flow through the column was 1.2 mL/min and the oven programmed from 40°C (held 5 min), ramped at 10°C/min to 230°C (held for 2 min), with a post run at 240°C (held for 2 min). The total run time was 30 minutes.
The MS was operated in electron impact (EI) mode (70 eV) using Selected Ion Monitoring (SIM), simultaneously acquiring scan data as well. In SIM mode the following m/z fragments were monitored: α-terpineol (IS) (59, 93, 136), 6-methyl-5-hepten-2-one (MHO) (69, 111, 126), geranyl acetone (69, 136, 121), α-ionone (121, 136, 192), β-ionone (136, 177, 192) and pseudo-ionone (81, 109, 135). Compound identification was performed by both comparisons of the retention times with that of authentic standards and the NIST2005 mass spectral library (National Institute of Standards, USA). Peaks of interest were quantified by external standard curves of the authentic standards. Data were normalised to the internal standard concentration (α-terpineol) and to the OD600 of the bacterial cultures before HS-SPME analysis.
Chemical analysis of leaf photosynthetic pigments and volatile apocarotenoids
Photosynthetic pigments of leaves were analysed using the method described in Lashbrooke et al..
Leaf volatiles were extracted according to the method described by Lücker et al. with modifications. Frozen, ground leaf tissue (200 mg) was placed in a 20 mL SPME vial and 10 mL of 20% (w/v) NaCl containing 160 ng 3-octanol (as internal standard, IS). The vial was sealed with a PTFE/silicon septum. Samples in sealed SPME vials were heated to 80°C and incubated for 5 minutes before the injection needle was pierced through the septum exposing the divinylbenzene/Carboxen/polydimethylsiloxane (DVB/CAR/PDMS) 50/30 μm coated solid phase microextraction (SPME) fibre (Supelco, Belfonte, PA, USA) to the headspace of the sample. During extraction the sample was stirred at 500 rpm and maintained at 80°C. After 15 minutes the fibre was removed and injected into the GC inlet where it was desorbed for 10 minutes at 260°C.
Extracts were analysed using an Agilent 6890 Gas Chromatograph coupled to a Waters GCT Time of Flight (TOF) Mass Spectrometer (MS) (Waters Corporation, Milford, MA, USA) Waters Masslynx GC/MS workstation software were used to analyse the data. The injector port was heated to 260°C and splitless injection (with a purge time of 3 minutes) was used. Separation was performed on an HP5MS (Agilent Technologies, Palo Alto, CA) column (30 mL × 0.25 mm i.d. × 0.25 μm f.t.) with helium as the carrier gas at a constant flow of 1 mL.min-1. The initial oven temperature was 40°C for 5 minutes, after which the temperature was increased by 5°C.min-1 to 150°C and then at 10°C.min-1 to 280°C (held for 2 minutes). Ionisation was in electron impact mode with an electron energy of 70 eV. The MS detector was set as follows: The transfer line, ion source and trap temperatures were 250, 180 and 150°C, respectively. The mass range was 35 to 650 m/z, with a scan rate of 4 scans.s-1. Compound identification was performed by both comparisons to the retention times of authentic standards and to the NIST05 mass spectral library (National Institute of Standards, USA).
Putative CCD-encoding gene isolation and characterisation
A phylogenetic tree of the CCD family from A. thaliana and V. vinifera and based on protein similarity is shown in Figure 1. From the molecular phylogenetic analysis five clades can be distinguished that correspond to the various orthologous groups (corresponding to the enzymatic function), namely: NCED, CCD1, CCD4, CCD7 and CCD8. In this study, three putative VvCCD encoding genes (VvCCD1 [GenBank:KF008001], VvCCD4a [GenBank:KF008002] and VvCCD4b [GenBank:KF008003]) were isolated from V. vinifera L. cv Pinotage cDNA using primers described in Additional file 1.
VvCCD1 is present in the grape genome as a tandem duplication on chromosome 13 . The two gene copies are situated approximately 78 kb from each other and show 96% identity at the nucleic acid level and a 97% identity on the amino acid level. Further, the 8.8 kb genomic regions of the genes (including introns and UTRs) share a 96% identity at the nucleic acid level. This suggests that the VvCCD1 isomers are functional equivalents and are treated as such in further experiments. RNAi constructs were designed to silence both isomers while real time primers did not distinguish between the two transcripts. Southern blot analysis of VvCCD1 confirmed that V. vinifera cv. Sultana genomic DNA possesses two copies of the gene (Additional file 3). According to the genome sequence CCD4a and CCD4b are within 26 kb of each other on chromosome 2; both genomic copies consist of a single exon (i.e. no introns) and code for 599 aa and 589 aa proteins, respectively, sharing 70% identity on amino acid level.
An additional CCD4 orthologue (VvCCD4c) was identified through sequence similarity and was localised to chromosome 16, however expression of this orthologue could not be detected in any of the tissues analysed and it was therefore not isolated.
In silico protein localisation predicted a cytosolic localisation for VvCCD1 and a plastidial localisation for VvCCD4a and VvCCD4b (Additional file 4). Protein alignments between CCD orthologues display a highly conserved amino acid sequence (Additional file 5). Four crucial histidine residues that are conserved in CCD orthologues were identified in VvCCD1, VvCCD4a and VvCCD4b (Additional file 4 and Additional file 5) . These amino acids are involved in the binding of an iron cation (Fe2+) which has been shown to be a co-factor for the carotenoid cleavage reaction .
Functionality of the putative VvCCD enzymes in Escherichia coli
To determine the enzymatic function of the isolated putative CCD-encoding genes; the coding regions were cloned into an E. coli expression vector (pTWIN1). The recombinant proteins were co-expressed in carotenoid accumulating E. coli strains engineered to accumulate specific carotenoids: phytoene (via pAC-PHYT), ζ-carotene (via pAC-ZETA), neurosporene (via pAC-NEUR), lycopene (via pAC-LYC), ϵ-carotene (via pAC-EPSILON) and β-carotene (via pAC-BETA) strains as described in Cunningham et al.[32, 33]. Where possible, carotenoid production in the strains used was verified using UPLC (Additional file 6). Enzyme activities were monitored after induction of the recombinant CCD proteins in the carotenoid-accumulating strains by measuring the formation of the volatile apocarotenoid cleavage products via headspace (HS)-SPME GC/MS.
The data, as presented in Figure 2 and Additional file 6, shows that VvCCD1, VvCCD4a and VvCCD4b are functional and have unique substrate preferences/specificities. VvCCD1, VvCCD4a and VvCCD4b all catalysed lycopene cleavage (to form 6-methyl-5-hepten-2-one; MHO) and ϵ-carotene (to form α-ionone). Neurosporene cleavage was catalysed by only VvCCD4a and VvCCD4b (not by VvCCD1). Only VvCCD1, however, catalysed β-carotene cleavage to form β-ionone; and only VvCCD4b catalysed ζ-carotene cleavage to form geranyl acetone. None of the three CCDs demonstrated an ability to catalyse the cleavage of phytoene. The production of α-ionone from ϵ-carotene provides evidence that VvCCD1, VvCCD4a and VvCCD4b possess the ability to catalyse 9,10(9’,10’) cleavage, whereas the formation of 6-methyl-5-hepten-2-one from lycopene demonstrates additional catalysis of 5,6(5’,6’) cleavage.
Spatial and temporal expression of CCDs in grapevine organs
The expression levels of VvCCD1, VvCCD4a, VvCCD4b, VvCCD4c, VvCCD7 and VvCCD8 were analysed in leaves, flowers and three grape berry developmental stages: green, véraison and ripe (Figure 3 and Additional file 7). No expression could be detected for VvCCD4c, VvCCD7 or VvCCD8 in any of the tissues or developmental stages tested using a qRT-PCR assay (results not shown), and therefore only expression of VvCCD1, -4a and -4b are reported and discussed further. The data shows that the VvCCDs were expressed in all tissues analysed. Specific patterns were, however, evident in the expression profiles: VvCCD1 expression appeared constitutive with the highest relative levels in leaves. VvCCD4a was most abundant in leaves; whereas VvCCD4b expression was highest in berries. VvCCD1, VvCCD4a and VvCCD4b were all expressed in flower tissue at relatively low levels.
The lowest relative expression levels for VvCCD1, VvCCD4a and VvCCD4b were all in young (green) berries. The highest VvCCD1 and VvCCD4a expression levels were in leaf tissue; whereas the highest expression for VvCCD4b was in ripe berries (Figure 3 and Additional file 7). VvCCD1, VvCCD4a and VvCCD4b expression all increased with development (ripening) in the berry stages. VvCCD1 and VvCCD4a expression peaked and levelled off at véraison, whereas VvCCD4b expression increased dramatically throughout berry ripening.
Transgenic manipulation of VvCCD1 levels
Transformation of V vinifera L. cv Sultana with a pART27-VvCCD1 overexpression cassette, was confirmed by Southern hybridisation (Additional file 3). Digestion of genomic DNA with SpeI resulted in a single hybridisation band per integration event as the restriction enzyme digests outside of the zone of hybridisation. Analysis of the transgenic plants showed that six of the nine lines represented independent integration events, with a transgene copy number ranging between one and four. The CCD1-10 and CCD1-12 lines, as well as the CCD1-15, CCD1-17, and CCD1-19 lines were considered clonal (Additional file 3). Twelve lines were shown to be positive for transformation/integration of the transgene with a silencing cassette via PCR screening (data not shown).
The level of VvCCD1 expression in the transgenic lines was monitored via qRT-PCR. Of the six lines independently transformed with pART27-VvCCD1, only two lines showed significant overexpression of VvCCD1 (up to an 85% increase relative to the expression seen in wild-type) (Figure 4). qRT-PCR expression analysis demonstrated transcription of the endogenous gene as well as the introduced transgene in all the lines, yet four lines displayed total VvCCD1 gene expression levels which were not significantly increased (when compared to the wild-type) (Figure 4). It is interesting to note that the transgene-derived expression was fairly constant whereas the endogenous gene expression was more affected. Of the twelve lines positively transformed with pART27-CCD1(RNAi), seven showed significant silencing when compared to the wild-type lines (Figure 4). Silencing of VvCCD1 of up to 85% (relative to wild-type expression) was observed. Targeted metabolite analyses were performed on plant lines with expression levels that differed significantly from the wild-type to determine if the carotenoid (i.e. the cleavage substrates) and/or the volatile apocarotenoid profiles (i.e. cleavage products) were affected/altered.
Carotenoid, chlorophyll and apocarotenoid analysis of transgenic grapevine lines
RP-HPLC analysis of pigments extracted from the transgenic population showed no significant correlation between VvCCD1 expression levels and the concentration of carotenoids in grapevine leaf tissue under the conditions tested (Additional file 8). Similarly, no correlation between VvCCD1 expression and leaf norisoprenoid levels were observed in the same tissue (Additional file 9). Total carotenoid content however, showed strong positive correlation to the total chlorophyll content of the leaves (R2 = 0.90) (Figure 5).
VvCCD1, VvCCD4a and VvCCD4b catalyse the cleavage of a broad range of carotenoid substrates
The enzymatic catalysation of the cleavage of carotenoids by CCDs has been shown to produce volatile flavour and aroma apocarotenoids including α-ionone, β-ionone and 6-methyl-5-hepten-2-one (MHO) in a range of plant species. Apocarotenoids contribute to the floral and fruity attributes of many wine cultivars and are thereby partly responsible for the “varietal character” of grapes and wine (e.g. Chenin blanc, Semillon, Sauvignon blanc, Cabernet Sauvignon, and Shiraz). Here we confirmed the functionality of VvCCD1, and for the first time VvCCD4a and VvCCD4b on a range of carotenoid substrates. The identification of CCD4 orthologues from grapevine has recently been reported [6, 38]; and Guillaumie et al. tested a CCD4a isolated from V. vinifera cv Chardonnay on ζ-carotene, lycopene, β-carotene, and zeaxanthin, but could not show functionality on any of the substrates tested. CCD1 and CCD4 orthologues in other plant species have been shown to catalyse cleavage of a number of C40-carotenoid and C30-apocarotenoid substrates. Here we show VvCCD1, VvCCD4a and VvCCD4b are capable of catalysis of the cleavage of C40 carotenoid substrates at the 9, 10 (9’, 10’) (ζ-carotene, β-carotene and/or ϵ-carotene) and lycopene at the 5, 6 (5’, 6’) double bond position to release the corresponding C13 apocarotenoid products (Table 1 and Figure 6), confirming cleavage of both cyclic and linear substrates. This is the first example of a CCD4 enzyme catalysing the cleavage of linear carotenoids and is in contrast to the conclusions made by Huang et al. who, after analysing the functionality of CCD4s from five different plant species (excluding grapevine) concluded that CCD4s catalyse the cleavage of cyclic non-polar carotenoids (e.g. β-carotene) and not linear carotenoids (e.g. lycopene or ζ-carotene). Interestingly, only VvCCD4b catalysed the cleavage of ζ-carotene and neither VvCCD4a nor VvCCD4b could catalyse β-carotene cleavage. None of the CCDs tested catalysed the cleavage of phytoene. These results are in agreement with the hypothesis by Vogel et al., who suggest that CCD-catalysed cleavage only occurs when a double bond is found adjacent to the bond that is to be cleaved. In the case of 5, 6 (5’, 6’) or 9, 10 (9’, 10’) cleavage a double bond must therefore be found at the 7, 8 (7’, 8’) or 11, 12 (11’, 12’) positions, respectively. Phytoene does not possess these double bonds and is therefore not cleaved. The ability of VvCCD4b to catalyse the cleavage of ζ-carotene to form geranylacetone, but not MHO, further illustrates this point (Figure 6). Carotenoids containing hydroxyl groups (e.g. lutein and zeaxanthin) as potential substrates for the VvCCD4 catalysed cleavage were not investigated in our study and remains to be evaluated.
Mathieu et al. used an in vitro enzyme assay to demonstrate that a VvCCD1 from V. vinifera L. cv Shiraz catalysed the cleavage of the xanthophylls zeaxanthin and lutein to form 3-hydroxy-β-ionone. The authors stated that β-carotene was tested as a substrate, but that it was not cleaved in their assay. VvCCD1 isolated from V. vinifera L. cv Pinotage in this study, however, was capable of catalysing the cleavage of lycopene, β-carotene and ϵ-carotene, but not neurosporene and ζ-carotene (Figure 2 and Figure 6). Cross-comparing results from different studies are often complicated by the differences in the assays utilised for experiments of this nature (i.e. in vivo versus in vitro enzyme assays) and/or the choice of analytical methods used to generate the data (i.e. degradation of carotenoids versus formation of apocarotenoids). One of the advantages of the in vivo assay used in this study is the controlling and validation of the specific carotenoid substrates. Carotenoid biosynthesis in the E. coli strains was controlled by the addition of the carotenoid pathway inhibitor diphenylamine (DPA; according to Cunningham and Gantt ) whereas the carotenoid(s) produced in the respective strains after 2 hours of DPA inhibition were verified by UPLC before induction of the respective CCDs. Steps were further taken to prevent the oxidative, non-enzymatic degradation of the carotenoids and a co-factor was added to ensure functionality of the CCD enzymes in the in vivo assays (according to Baldermann et al. ).
In vivofunctions of the isolated VvCCDs
VvCCD1, VvCCD4a and VvCCD4b influence the flavour and aroma potential of grapes
VvCCD1, -4a and 4b, were all up-regulated during ripening (Figure 3), and are therefore all potentially involved in the enzymatic degradation of carotenoids to the respective aromatic C13-norisoprenoids that contribute to the distinctive varietal character of grapes and wine. Since the VvCCD1, -4a and -4b are all expressed during ripening, the specific carotenoid substrate(s) available for cleavage, as well as the substrate specificity of the respective VvCCD(s) present, will determine the C13-norisoprenoid(s) formed in grapes. Although VvCCD1, VvCCD4a and VvCCD4b are expressed during berry development; VvCCD4b showed the most berry-specific expression profile and the highest upregulation throughout berry ripening (30-fold upregulation at the ripe stage relative to the green stage) and appears to be the isoform most likely responsible for catalysing carotenoid cleavage in ripening berries. VvCCD4a showed the highest expression in leaves and VvCCD1 maintains relatively constant levels in all tissues tested. In agreement with the expression data presented here, Mathieu et al. showed similar trends for VvCCD1 expression in berries (i.e. peaking at véraison), and, while the authors noted an increase in the C13-norisoprenoid content of Muscat (and to a lesser extent Shiraz), this occurred two weeks after the increase in VvCCD1 expression. Numerous studies on grape berry carotenoid composition have shown that carotenoid concentrations decrease during ripening [14, 43, 55]. The inverse correlation observed between carotenoids and C13-norisoprenoids lead Crupi et al. to propose that the change in carotenoid concentration in grape berries from véraison stage to the ripe (harvest) stages could be used to estimate the aromatic potential of the grapes.
VvCCD4a and VvCCD4b are candidates for maintenance of carotenoid levels during photosynthesis
The relative abundance of oxygenated carotenoids (xanthophylls) is conserved and tightly regulated in photosynthetic tissues and is largely due to the involvement of specific pigments in the photosynthetic reaction centres of Photosystems (PS) I and II (mainly β-carotene) and the light harvesting antennae complexes (mainly the xanthophylls lutein, violaxanthin, and neoxanthin).
Although carotenoid composition is considered highly conserved in photosynthetic organisms with the ubiquitous presence of the xanthophylls lutein, neoxanthin and violaxanthin most notable; mutant studies in A. thaliana have shown that a certain degree of plasticity is tolerated in plants. Plants have been shown to be viable even in the absence of lutein, neoxanthin and violaxanthin, but these xanthophylls are required for optimal seedling development and photoprotection, and surprisingly to a lesser extent photosynthesis .
The VvCCD1 transgenic lines also showed positive correlation between the concentrations of chlorophyll and carotenoids in mature photosynthetically active leaves (Figure 5; R2 = 0.90). This is expected as carotenoids are primarily involved in photosynthesis specifically in vegetative tissue . An increase in chlorophyll concentration is indicative of increased photosynthetic activity, which in turn puts more demand on the carotenoids involved in light-harvesting and photoprotection . It is therefore not surprising that the carotenoid pathway is tightly regulated in leaf tissue, as loss of these crucial pigments would lead to an impaired and consequently sub-optimal plant [58–61].
Beisel et al. demonstrated continuous synthesis and degradation of carotenoids and chlorophyll a in mature leaves of Arabidopsis. This turnover of carotenoids and chlorophylls appears crucial for the maintenance of active photosynthesis and for adaptation to changing light conditions. It is possible that the CCDs (especially chloroplast localised CCD4 orthologues) are involved in the maintenance of the optimal carotenoid composition in photosynthetic tissue. Static plants confronted with an ever-changing environment must be capable of maintaining an optimal carotenoid composition in photosynthetic tissues. Due to their localisation and substrate specificities, CCDs may be involved in this regulation and maintenance. We show that the cytosolic VvCCD1 catalyses lycopene, β-carotene and ϵ-carotene (but not ζ-carotene) cleavage (Figure 2), whereas the chloroplast localised VvCCD4a and VvCCD4b catalyses lycopene, neurosporene and ϵ-carotene (but not β-carotene) cleavage (Figure 2). Only VvCCD4b was able to catalyse ζ-carotene cleavage. Of these carotenoid substrates, only β-carotene is present at detectable levels in grapevine leaves and berries (Figure 3 and Additional file 7), where it forms part of photosystem I and –II. Differential transcriptional regulation and the physical separation of the carotenoid substrates (chloroplastic) from the VvCCD1 enzyme (cytosolic) therefore add additional layers of possible control.
Altering the expression of VvCCD1in transgenic grapevine suggests sub-cellular compartmentalisation regulates CCD activity
Our transgenic data confirmed a level of protection from manipulation of the carotenoid pathway, specifically from altered levels of VvCCD1. Significant overexpression of the VvCCD1 was only observed in 30% of the Southern positive grapevine lines. This was not due to a non-functional construct, since qRT-PCR experiments verified endogenous and the transgenic VvCCD1 expression in the plant lines (Figure 4). In spite of the partial silencing of most of the overexpression lines (by controlling the endogenous gene expression level); lines were generated that exhibited varying degrees of overexpression of VvCCD1 (Figure 4). The overexpressing lines, together with the lines that showed successful silencing, resulted in a population of transgenic plants that exhibited an up to ~12-fold range of VvCCD1 expression (from the most silenced line to the most overexpressed line).
Despite this range in VvCCD1 expression no direct phenotype was observed in the vegetative (leaf) tissue tested for either the carotenoids (substrates) or apocarotenoids (products) based on known VvCCD1 enzyme activity. Mathieu et al. monitored ripening berries and found a similar discrepancy (or lack of correlation) between VvCCD1 expression and apocarotenoid production. Since quantification of the VvCCD1 protein was not performed on the transgenic lines, it is not possible to speculate on the relationship between VvCCD1 transcripts and VvCCD1 protein, but it is known that a positive correlation between mRNA levels and protein levels is far less common than often assumed . Another factor that could contribute to the lack of an observable phenotype in the leaf tissue analysed, is the compartmentalisation of the enzymes within a plant cell. In silico analysis suggest that VvCCD1 is localised in the cytosol. This has been shown to be the case for many CCD1 orthologues . The carotenoid cleavage substrates that CCD1 has been shown to catalyse in vitro, however, are situated in the chloroplast membrane, and are thus inaccessible to the CCD1 enzyme .
Previous attempts to manipulate the expression levels of CCD1 transcripts have also led to phenotypes inconsistent with the observed in vitro activity of CCD1 [18, 19]. Simkin et al. reduced LeCCD1 mRNA levels by up to 90% in tomato leaves and fruit using an antisense construct, but did not observe any change in the carotenoid concentration in fruit with reduced CCD1 levels, and only a 50% decrease in the β-ionone concentration in selected silenced lines. No data was presented for carotenoid or norisoprenoid levels in tomato leaves with reduced CCD1 levels. Ilg et al. suggested that in planta OsCCD1 may catalyse apocarotenoid cleavage rather than carotenoids. A similar reduction of the norisoprenoids observed in tomato fruit with reduced CCD1 transcripts was not seen in grapevine leaves (Additional file 9). These studies, and supported by the results presented in this study, suggest that the in planta role of CCD1 may in fact not be maintenance of carotenoid levels, but catalysing apocarotenoid cleavage. It is not surprising when considering that the leaf is the primary photosynthetic organ of the plant and therefore needs to maintain this function. The correlation observed between chlorophyll concentration and carotenoid concentration in the leaf (Figure 5) indicates that the level of photosynthetic activity of the tissue has a much greater influence on the concentration of carotenoids. In the chromoplasts of ripe fruit the need for photoprotection of the chlorophylls is absent and the segregation of CCD1 and its carotenoid substrates is possibly diminished. However, despite the predicted cytosolic localisation of CCD1 and its apparent lack of transcript correlation with carotenoid and norisoprenoid concentrations, norisoprenoids are still formed in the leaves (Additional file 9). This suggests another mechanism of action for the cleavage of carotenoids and the production of norisoprenoids. The CCD4s are the most likely candidates due to the fact that the VvCCD4a and VvCCD4b transcripts are upregulated during berry development (peaking at harvest for VvCCD4b); subcellularly both VvCCD4a and VvCCD4b are predicted to co-localise with carotenoids in the chloroplast; and the catalysis of carotenoid cleavage by VvCCD4a and VvCCD4b have been demonstrated.
On a sub-organellar level, a number of carotenoid metabolic enzymes have been identified in the plastoglobule proteome of A. thaliana, including CCD1 and CCD4. Interestingly the CCD4 protein represented 3.3% of the total mass of the plastoglobule proteome . Plastoglobules are thylakoid-associated lipoprotein particles found in plastids (i.e. suborganellar compartmentalisation). It is thought that lipid exchange (i.e. carotenoids, plastoquinones, tocopherols) can occur between the plastoglobules and the thylakoid membrane. The size and abundance of plastoglobules in chloroplasts are affected by a number of developmental and environmental conditions, and includes stresses (especially oxidative) and transitions from chloroplasts to gerontoplasts (i.e. senescence) and chloroplast to chromoplast transitions (e.g. as occurs in flowers and fruit).
Plastids can differentiate and dedifferentiate and the size and number of plastoglobules increases during these transitions. It is interesting to note that CCD1, CCD4 and CCD8 have been localised to plastoglobules; and that the carotenoid substrates accumulate, and can be formed de novo in plastoglobules. The in planta role of the CCDs in these lipoprotein structures is still not clear. If they are required to maintain the carotenoid composition and/or it is for the production of the apocarotenoid cleavage product that drives carotenoid cleavage remains to be elucidated.
To summarise, VvCCD1 in grapevine leaves appears to be under various levels of control. All factors being considered, the importance of the carotenoid composition for effective photosynthesis is the most likely reason for this control in the leaf. The control is applied at the transcript level, where a form of post-transcriptional gene silencing was observed in the transgenic VvCCD1 population; and possibly on the protein level, where sub-cellular compartmentalisation may prevent interaction between VvCCD1 and its carotenoid substrate(s). The substrate specificity of the respective VvCCDs characterised in this study (i.e. VvCCD1, VvCCD4a and VvCCD4b), suggest another level where control can be exerted. Despite the fact that VvCCD1 has the ability to catalyse the cleavage of multiple carotenoids in vitro, the in planta substrates for cleavage may be primarily C27 apocarotenoids produced through cleavage by enzymatic action (by CCD4 and/or CCD7 as suggested by Floss et al. or photo-oxidation, and subsequently transported from the chloroplast to the cytosol. In either case grape berries would likely display a phenotype more closely correlated to VvCCD1 expression due to the increased osmotic stress that occurs during ripening, resulting in leaky membranes and the concomitant degradation of chloroplasts. The extensive youth phase/maturation period in grapevine (a woody perennial) that can last in excess of three years, excluded the analysis of berries from the transgenic populations generated from the scope of this study.
The isolation and functional characterisation of VvCCD4a and VvCCD4b provides additional candidate cleavage enzymes affecting the carotenoid composition in the chloroplast, as well as the production of volatile apocarotenoids in grapevine. Their differential expression in various plant tissues and the differential substrate specificities of the VvCCD1, VvCCD4a and VvCCD4b suggests that CCDs have distinct roles in different plants, plant tissues and even different subcellular compartments of plants (i.e. plastids). Future studies on, for example, the senescing leaves and grape berries from the transgenic lines generated in this study will be of great importance in further elucidating the in planta function of CCDs. Generation of transgenic grapevine altered in VvCCD4 expression as well as future studies on the senescing leaves and grape berries from the transgenic lines generated in this study will be of great importance in further elucidating the in planta function of CCDs.
Availability of supporting data
The data sets supporting the results of this article are included within the article (and its additional files).
Cogdell RJ: Carotenoids in photosynthesis. Pure Appl Chem. 1985, 57: 723-728. 10.1351/pac198557050723.
Biswal B: Carotenoid catabolism during leaf senescence and its control by light. J Photochem Photobiol B. 1995, 30: 3-13. 10.1016/1011-1344(95)07197-A.
Britton G: Structure and properties of carotenoids in relation to function. FASEB J. 1995, 9: 1551-1558.
Cunningham FX: Regulation of carotenoid synthesis and accumulation in plants. Pure Appl Chem. 2002, 74: 1409-1417. 10.1351/pac200274081409.
Velasco R, Zharkikh A, Troggio M, Cartwright DA, Cestaro A, Pruss D, Pindo M, FitzGerald LM, Vezzulli S, Reid J, Malacarne G, Iliev D, Coppola G, Wardell B, Micheletti D, Macalma T, Facci M, Mitchell JT, Perazzolli M, Eldredge G, Gatto P, Oyzerski R, Moretto M, Gutin N, Stefanini M, Chen Y, Segala C, Davenport C, Dematté L, Mraz A, et al: A high quality draft consensus sequence of the genome of a heterozygous grapevine variety. PLoS One. 2007, 2: e1326-10.1371/journal.pone.0001326.
Young P, Lashbrooke J, Alexandersson E, Jacobson D, Moser C, Velasco R, Vivier M: The genes and enzymes of the carotenoid metabolic pathway in Vitis vinifera L. BMC Genomics. 2012, 13: 243-10.1186/1471-2164-13-243.
Auldridge ME, McCarty DR, Klee HJ: Plant carotenoid cleavage oxygenases and their apocarotenoid products. Curr Opin Plant Biol. 2006, 9: 315-321. 10.1016/j.pbi.2006.03.005.
Auldridge ME, Block A, Vogel JT, Dabney-Smith C, Mila I, Bouzayen M, Magallanes-Lundback M, DellaPenna D, McCarty DR, Klee HJ: Characterization of three members of the Arabidopsis carotenoid cleavage dioxygenase family demonstrates the divergent roles of this multifunctional enzyme family. Plant J. 2006, 45: 982-993. 10.1111/j.1365-313X.2006.02666.x.
Chernys JT, Zeevaart JAD: Characterization of the 9-cis-epoxycarotenoid dioxygenase gene family and the regulation of abscisic acid biosynthesis in avocado. Plant Physiol. 2000, 124: 343-353. 10.1104/pp.124.1.343.
Dun EA, Brewer PB, Beveridge CA: Strigolactones: discovery of the elusive shoot branching hormone. Trends Plant Sci. 2009, 14: 364-372. 10.1016/j.tplants.2009.04.003.
Huang FC, Molnar P, Schwab W: Cloning and functional characterization of carotenoid cleavage dioxygenase 4 genes. J Exp Bot. 2009, 60: 3011-3022. 10.1093/jxb/erp137.
Baldermann S, Naim M, Fleischmann P: Enzymatic carotenoid degradation and aroma formation in nectarines (Prunus persica). Food Res Int. 2005, 38: 833-836. 10.1016/j.foodres.2005.02.009.
Cooper CM, Davies NW, Menary RC: Changes in some carotenoids and apocarotenoids during flower development in Boronia megastigma (Nees). J Agric Food Chem. 2009, 57: 1513-1520. 10.1021/jf802610p.
Baumes R, Wirth J, Bureau S, Gunata Y, Razungles A: Biogeneration of C13-norisoprenoid compounds: experiments supportive for an apo-carotenoid pathway in grapevines. Anal Chim Acta. 2002, 458: 3-14. 10.1016/S0003-2670(01)01589-6.
Crupi P, Coletta A, Milella RA, Palmisano G, Baiano A, La Notte E, Antonacci D: Carotenoid and chlorophyll-derived compounds in some wine grapes grown in Apulian region. J Food Sci. 2010, 75: S191-S198. 10.1111/j.1750-3841.2010.01564.x.
Ristic R, Bindon K, Francis L, Herderich M, Iland P: lavonoids and C13-norisoprenoids in Vitis vinifera L. cv. Shiraz: relationships between grape and wine composition, wine colour and wine sensory properties. Aust J Grape Wine Res. 2010, 16: 369-388. 10.1111/j.1755-0238.2010.00099.x.
Mendes-Pinto MM: Carotenoid breakdown products the-norisoprenoids-in wine aroma. Arch Biochem Biophys. 2009, 483: 236-245. 10.1016/j.abb.2009.01.008.
Simkin AJ, Schwartz SH, Auldridge M, Taylor MG, Klee HJ: The tomato carotenoid cleavage dioxygenase 1 genes contribute to the formation of the flavor volatiles beta-ionone, pseudoionone, and geranylacetone. Plant J. 2004, 40: 882-892. 10.1111/j.1365-313X.2004.02263.x.
Floss DS, Schliemann W, Schmidt J, Strack D, Walter MH: RNA interference-mediated repression of MtCCD1 in mycorrhizal roots of Medicago truncatula causes accumulation of C27 apocarotenoids, shedding light on the functional role of CCD1. Plant Physiol. 2008, 148: 1267-1282. 10.1104/pp.108.125062.
Ilg A, Yu Q, Schaub P, Beye P, Al-Babili S: Overexpression of the rice carotenoid cleavage dioxygenase 1 gene in golden rice endosperm suggests apocarotenoids as substrates in planta. Planta. 2010, 232: 691-699. 10.1007/s00425-010-1205-y.
Walter MW, Strack D: Carotenoids and their cleavage products: biosynthesis and functions. Nat Prod Rep. 2011, 28: 663-692. 10.1039/c0np00036a.
Ytterberg AJ, Peltier JB, van Wijk KJ: Protein profiling of plastoglobules in chloroplasts and chromoplasts. A surprising site for differential accumulation of metabolic enzymes. Plant Physiol. 2006, 140: 984-997. 10.1104/pp.105.076083.
Rubio A, Rambla JL, Santaella M, Gómez MD, Orzaez D, Granell A, Gómez-Gómez L: Cytosolic and plastoglobule-targeted carotenoid dioxygenases from Crocus sativus are both involved in β-ionone release. J Biol Chem. 2008, 283: 24816-24825. 10.1074/jbc.M804000200.
Vallabhaneni R, Bradbury LMT, Wurtzel ET: The carotenoid dioxygenase gene family in maize, sorghum, and rice. Arch Biochem Biophys. 2010, 504: 104-111. 10.1016/j.abb.2010.07.019.
Vogel JT, Tan BC, McCarty DR, Klee HJ: The carotenoid cleavage dioxygenase 1 enzyme has broad substrate specificity, cleaving multiple carotenoids at two different bond positions. J Biol Chem. 2008, 283: 11364-11373. 10.1074/jbc.M710106200.
Altschul SF, Gish W, Miller W, Myers EW, Lipman DJ: Basic local alignment search tool. J Mol Biol. 1990, 215: 403-410.
Proost S, Van Bel M, Sterk L, Billiau K, Van Parys T, Van de Peer Y, Vandepoele K: PLAZA: a comparative genomics resource to study gene and genome evolution in plants. Plant Cell. 2009, 21: 3718-3731. 10.1105/tpc.109.071506.
Tamura K, Dudley J, Nei M, Kumar S: MEGA4: molecular evolutionary genetics analysis (MEGA) software version 4.0. Mol Biol Evol. 2007, 24: 1596-1599. 10.1093/molbev/msm092.
Steenkamp J, Wiid I, Lourens A, Vanhelden P: Improved method for DNA extraction from Vitis vinifera. Am J Enol Vitic. 1994, 45: 102-106.
Reid K, Olsson N, Schlosser J, Peng F, Lund S: An optimized grapevine RNA isolation procedure and statistical determination of reference genes for real-time RT-PCR during berry development. BMC Plant Biol. 2006, 6: 27-10.1186/1471-2229-6-27.
Sambrook J, Fritsch EF, Maniatis T: Molecular cloning: A laboratory manual. 2nd edition. Cold Spring Harbor N.Y: Cold Spring Harbor Laboratory Press; 1989.
Cunningham FX, Chamovitz D, Misawa N, Gantt E, Hirschberg J: Cloning and functional expression in Escherichia coli of a cyanobacterial gene for lycopene cyclase, the enzyme that catalyzes the biosynthesis of β-carotene. FEBS Lett. 1993, 328: 130-138. 10.1016/0014-5793(93)80980-9.
Cunningham FX, Sun Z, Chamovitz D, Hirschberg J, Gantt E: Molecular structure and enzymatic function of lycopene cyclase from the cyanobacterium Synechococcus sp strain PCC7942. Plant Cell. 1994, 6: 1107-1121.
Gleave AP: A versatile binary vector system with A T-DNA organizational-structure conducive to efficient integration of cloned DNA into the plant genome. Plant Mol Biol. 1992, 20: 1203-1207. 10.1007/BF00028910.
Wesley SV, Helliwel CA, Smith NA, Wang M, Rouse DT, Liu G, Gooding PS, Singh SP, Abbott D, Stoutjesdijk PA, Robinson SP, Gleave AP, Green AG, Waterhouse PM: Construct design for efficient, effective and high throughput gene silencing in plants. Plant J. 2001, 27: 581-590. 10.1046/j.1365-313X.2001.01105.x.
Vasanth K, Vivier MA: Optimisation of improved cryopreservation procedure for long term storage synchronised culture of grapevine (Vitis vinifera L.). Biol Plant. 2011, 55 (2): 365-369. 10.1007/s10535-011-0056-0.
Franks T, He DG, Thomas M: Regeneration of transgenic Vitis vinifera L. Sultana plants: genotypic and phenotypic analysis. Mol Breed. 1998, 4: 321-333. 10.1023/A:1009673619456.
Guillaumie S, Fouquet R, Kappel C, Camps C, Terrier N, Moncomble D, Dunlevy JD, Davies C, Boss PK, Delrot S: Transcriptional analysis of late ripening stages of grapevine berry. BMC Plant Biol. 2011, 11: 165-10.1186/1471-2229-11-165.
Pfaffl MW: A new mathematical model for relative quantification in real-time RT-PCR. Nucleic Acids Res. 2001, 29: 2002-2007.
Lücker J, Bouwmeester HJ, Schwab W, Blaas J, van der Plas LHW, Verhoeven HA: Expression of Clarkia S-linalool synthase in transgenic petunia plants results in the accumulation of S-linalyl-β-D-glucopyranoside. Plant J. 2001, 27: 315-324. 10.1046/j.1365-313x.2001.01097.x.
Cunningham FX, Gantt E: A portfolio of plasmids for identification and analysis of carotenoid pathway enzymes: Adonis aestivalis as a case study. Photosynthetic Res. 2007, 92: 245-259. 10.1007/s11120-007-9210-0.
Baldermann S, Kato M, Kurosawa M, Kurobayashi Y, Fujita A, Fleischmann P, Watanabe N: Functional characterization of a carotenoid cleavage dioxygenase 1 and its relation to the carotenoid accumulation and volatile emission during the floral development of Osmanthus fragrans Lour. J Exp Bot. 2010, 61: 2967-2977. 10.1093/jxb/erq123.
Lashbrooke JG, Young PR, Strever AE, Stander C, Vivier MA: The development of a method for the extraction of carotenoids and chlorophylls from grapevine leaves and berries for HPLC profiling. Aust J Grape Wine Res. 2010, 16: 349-360. 10.1111/j.1755-0238.2010.00097.x.
Kloer DP, Schulz GE: Structural and biological aspects of carotenoid cleavage. Cell Mol Life Sci. 2006, 63: 2291-2303. 10.1007/s00018-006-6176-6.
Poliakov E, Gentleman S, Cunningham FXJ, Miller-Ihli NJ, Redmond TM: Key role of conserved histidines in recombinant mouse beta-carotene 15,15'-monooxygenase-1 activity. J Biol Chem. 2005, 280: 29217-29223. 10.1074/jbc.M500409200.
Schwartz SH, Qin XQ, Zeevaart JAD: Characterization of a novel carotenoid cleavage dioxygenase from plants. J Biol Chem. 2001, 276: 25208-25211. 10.1074/jbc.M102146200.
Schmidt H, Kurtzer R, Eisenreich W, Schwab W: The carotenase AtCCD1 from Arabidopsis thaliana is a dioxygenase. J Biol Chem. 2006, 281 (15): 9845-9851. 10.1074/jbc.M511668200.
Ibdah M, Azulay Y, Portnoy V, Wasserman B, Bar E, Meir A, Burger Y, Hirschberg J, Schaffer AA, Katzir N, Tadmor Y, Lewinsohn E: Functional characterization of CmCCD1, a carotenoid cleavage dioxygenase from melon. Phytochemistry. 2006, 67: 1579-1589. 10.1016/j.phytochem.2006.02.009.
Mathieu S, Bigey F, Procureur J, Terrier N, Gunata Z: Production of a recombinant carotenoid cleavage dioxygenase from grape and enzyme assay in water-miscible organic solvents. Biotechnol Lett. 2007, 29: 837-841. 10.1007/s10529-007-9315-8.
Bouvier F, Suire C, Mutterer J, Camara B: Oxidative remodeling of chromoplast carotenoids: Identification of the carotenoid dioxygenase CsCCD and CsZCD genes involved in Crocus secondary metabolite biogenesis. Plant Cell. 2003, 15: 47-62. 10.1105/tpc.006536.
García-Limones C, Schnäbele K, Blanco-Portales R, Luz Bellido M, Caballero JL, Schwab W, Muňoz-Blanco J: Functional characterization of FaCCD1: a carotenoid cleavage dioxygenase from strawberry involved in Lutein degradation during fruit ripening. J Agric Food Chem. 2009, 56: 9277-9285.
Ohmiya A, Kishimoto S, Aida R, Yoshioka S, Sumitomo K: Carotenoid cleavage dioxygenase (CmCCD4a) contributes to white color formation in Chrysanthemum petals. Plant Physiol. 2006, 142: 1193-1201. 10.1104/pp.106.087130.
Campbell R, Ducreux LJM, Morris WL, Morris JA, Suttle JC, Ramsay G, Bryan GJ, Hedley PE, Taylor MA: The metabolic and developmental roles of carotenoid cleavage dioxygenase4 from potato. Plant Physiol. 2010, 154: 656-664. 10.1104/pp.110.158733.
Mathieu S, Terrier N, Procureur J, Bigey F, Günata Z: Carotenoid cleavage dioxygenase from vitis vinifera L.: functional characterization and expression during grape berry development in relation to C13 norisoprenoid accumulation. J Exp Bot. 2005, 56: 2721-2731. 10.1093/jxb/eri265.
Razungles AJ, Babic I, Sapis JC, Bayonove CL: Particular behavior of epoxy xanthophylls during véraison and maturation of grape. J Agric Food Chem. 1996, 44: 3821-3825. 10.1021/jf960260t.
Pogson BJ, Niyogi KK, Bjorkman O, DellaPenna D: Altered xanthophyll compositions adversely affect chlorophyll accumulation and nonphotochemical quenching in Arabidopsis mutants. Proc Natl Acad Sci USA. 1998, 95: 13324-13329. 10.1073/pnas.95.22.13324.
Lichtenthaler HK, Buschmann C, Döll M, Fietz H-J, Bach T, Kozel U, Meier D, Rahmsdorf U: Photosynthetic activity, chloroplast ultrastructure, and leaf characteristics of high-light and low-light plants and of sun and shade leaves. Photosynth Res. 1981, 2: 115-141. 10.1007/BF00028752.
Fraser PD, Enfissi EM, Bramley PM: Genetic engineering of carotenoid formation in tomato fruit and the potential application of systems and synthetic biology approaches. Arch Biochem Biophys. 2008, 483: 196-204.
Hirschberg J: Carotenoid biosynthesis in flowering plants. Curr Opin Plant Biol. 2001, 4: 210-218. 10.1016/S1369-5266(00)00163-1.
Toledo-Ortiz G, Huq E, Rodríguez-Concepción M: Direct regulation of phytoene synthase gene expression and carotenoid biosynthesis by phytochrome-interacting factors. Proc Natl Acad Sci USA. 2010, 107: 11626-11631. 10.1073/pnas.0914428107.
Welsch R, Beyer P, Hugueney P, Kleinig H, von Lintig J: Regulation and activation of phytoene synthase, a key enzyme in carotenoid biosynthesis, during photomorphogenesis. Planta. 2000, 211: 846-854. 10.1007/s004250000352.
Beisel KG, Jahnke S, Hofmann D, Köppchen S, Schurr U, Matsubara S: Continuous turnover of carotenes and chlorophyll a in mature leaves of Arabidopsis revealed by 14CO2 pulse-chase labeling. Plant Physiol. 2010, 152: 2188-2199. 10.1104/pp.109.151647.
Roberts JKM: Proteomics and a future generation of plant molecular biologists. Plant Mol Biol. 2002, 48: 143-154. 10.1023/A:1013736322130.
Lundquist PK, Poliakov A, Bhuiyan NH, Zybailov B, Sun Q, van Wijk KJ: The functional network of the Arabidopsis plastoglobule proteome based on quantitative proteomics and genome-wide coexpression analysis. Plant Physiol. 2012, 158: 1172-1192. 10.1104/pp.111.193144.
The authors wish to thank Dr Andreas Tredoux and Mr Lucky Mokwena for their assistance with the GC/MS analysis of the volatiles in the bacterial headspace and Dr Hans Eyéghé–Bickong for the UPLC analysis of carotenoids in the bacterial cultures.
This work was supported by grants from the Wine Industry Network for Expertise and Technology (Winetech), Technology and Human Resources for Industry Programme (THRIP), and the National Research Foundation (NRF).
The authors declare that they have no conflict of interest.
JGL, PRY and MAV conceptualised the study. JGL, PRY and MAV were involved in the experimental layout. JGL, PRY and SJD isolated and cloned the genes of interest and performed the bacterial functional complementation assays. JGL constructed the plant transformation constructs. KV performed the grapevine transformations and subsequent selection and regeneration of plantlets. JGL performed the genetic and metabolite screening of the transgenic plants. JGL, PRY and MAV drafted the initial manuscript. All authors contributed to the discussion of the results, reviewing of the manuscript and approved the final manuscript.
Electronic supplementary material
Additional file 3: Southern hybridisation confirming integration of pART27-VvCCD1. Band sizes (in bp) of λ DNA digested with BstE II (lane 1) is shown. Genomic DNA was digested with SpeI. Two hybridisation events in the wild-type (lane 2) indicate two copies of VvCCD1 in the Sultana genome. Lane 3, CCD1-01; lane 4, CCD1-02; lane 5, CCD1-10; lane 6, CCD1-12; lane 7, CCD1-14; lane 8, CCD1-15; lane 9, CCD1-17; lane 10, CCD1-18; lane 11, CCD1-19. Estimated number of integration events are displayed at the bottom of each lane. Plants with the same clonal group (a-f) are considered clonal copies. (PDF 114 KB)
Additional file 6: Functionality and substrate specificity of VvCCD1, VvCCD4a and VvCCD4b in a heterologous in vivo bacterial system. CCDs were expressed in Escherichia coli engineered to accumulate specific carotenoids. Carotenoids produced before cleavage were determined using UPLC. Volatile apocarotenoids produced after cleavage were determined using GC-MS. (PDF 215 KB)
Additional file 7: Carotenoids and chlorophyll concentrations present in the grapevine organs investigated in this study. Carotenoids and chlorophylls were analysed by HPLC. Individual carotenoids and chlorophylls were identified by comparison to authentic standards and quantified by normalisation to an internal standard (β-apo-carotenal) and quantified by external standard curve as described in Lashbrooke et al. (2010). (PDF 107 KB)
Additional file 8: Relationship between carotenoid concentration and VvCCD1 expression levels in grapevine leaves. None of the major carotenoids in the leaves of the grapevine population (measured via HPLC) showed significant correlation with VvCCD1 expression. The concentration of β-carotene (A), lutein (B), violaxanthin (C), neoxanthin (D), antheraxanthin (E) and zeaxanthin (F) found in wild-type (green triangle symbol), silenced (blue diamond symbol) and overexpression (red square symbol) lines is shown. (PDF 355 KB)
Additional file 9: Relationship between apocarotenoid concentration and VvCCD1 expression levels in grapevine leaves. No significant correlation was found between the VvCCD1 expression and volatile apocarotenoids in the leaves of the grapevine population (measured via GC/MS). The concentration of 6-methyl-5-hepten-2-one (MHO) (A), pseudoionone (B), α-ionone (C), β-ionone (D), and geranylacetone (E) found in wild-type (blue diamond symbol), silenced (red square symbol) and overexpression (light green triangle symbol) lines is shown. (PDF 348 KB)
Authors’ original submitted files for images
About this article
Cite this article
Lashbrooke, J.G., Young, P.R., Dockrall, S.J. et al. Functional characterisation of three members of the Vitis viniferaL. carotenoid cleavage dioxygenase gene family. BMC Plant Biol 13, 156 (2013). https://doi.org/10.1186/1471-2229-13-156
- Vitis vinifera L
- Cleavage dioxygenase