Reduced lignin content and altered lignin composition in the warm season forage grass Paspalum dilatatum by down-regulation of a Cinnamoyl CoA Reductase Gene
C4 grasses are favoured as forage crops in warm, humid climates. The use of C4 grasses in pastures is expected to increase because the tropical belt is widening due to global climate change. While the forage quality of Paspalum dilatatum (dallisgrass) is higher than that of other C4 forage grass species, digestibility of warm-season grasses is, in general, poor compared with most temperate grasses. The presence of thick-walled parenchyma bundle-sheath cells around the vascular bundles found in the C4 forage grasses are associated with the deposition of lignin polymers in cell walls. High lignin content correlates negatively with digestibility, which is further reduced by a high ratio of syringyl (S) to guaiacyl (G) lignin subunits. Cinnamoyl-CoA reductase (CCR) catalyses the conversion of cinnamoyl CoA to cinnemaldehyde in the monolignol biosynthetic pathway and is considered to be the first step in the lignin-specific branch of the phenylpropanoid pathway. We have isolated three putative CCR1 cDNAs from P. dilatatum and demonstrated that their spatio-temporal expression pattern correlates with the developmental profile of lignin deposition. Further, transgenic P. dilatatum plants were produced in which a sense-suppression gene cassette, delivered free of vector backbone and integrated separately to the selectable marker, reduced CCR1 transcript levels. This resulted in the reduction of lignin, largely attributable to a decrease in G lignin.
KeywordsC4 forage grass Cinnamoyl-CoA reductase Lignin Paspalum dilatatum
Dallisgrass (Paspalum dilatatum Poir.) is a C4 grass native to South America, but widely grown for forage in tropical, subtropical and warm temperate regions of the world. Several polyploid biotypes, including sexual tetraploids, apomictic pentaploids and hexaploids have been described (Casa et al. 2002). Valued for its vigour, dallisgrass produces yields of up to 15 tons of dry matter per hectare (Cook et al. 2005) with crude protein concentrations of up to 18.6 % (Baréa et al. 2007). It can withstand heavy grazing and is somewhat tolerant to frost and water stress (Hutton and Nelson 1968; Robinson et al. 1988).
With the widening of the tropical belt due to global climate change (for review see Seidel et al. (2008) the market for C4 forages grasses is set to increase. However, while the forage quality of P. dilatatum is higher than that of other C4 forage grass species, digestibility of warm-season grasses is, in general, poor compared with most temperate grasses (Wilson 1994). This is due to the presence of lignin deposits in the thick-walled parenchyma bundle-sheaths around each vascular bundle (Wilson 1993). Lignin acts as a physical barrier to the microbial enzymes that digest polysaccharides, limiting the achievable degradation of cellulose and hemicellulose and limiting the digestible energy available to ruminants (Jung and Allen 1995). Consequently, modification of the lignin biosynthetic pathway, either by analyses of mutants or by genetic modification, is of great interest (Gordon and Neudoerffer 1973; Barrière et al. 1994; Halpin et al. 1994; Bernard-Vailh et al. 1996; Guo et al. 2001; Chen et al. 2004; Li et al. 2008; Hisano et al. 2009; Tu et al. 2010).
Lignin, found in the cell walls of vascular plants, is a complex heteropolymer resulting from radical coupling reactions of three main monolignols: p-coumaryl alcohol, coniferyl alcohol and sinapyl alcohol. The degree of methoxylation of the phenyl ring differs in each subunit giving rise to hydroxyphenyl (H), guaiacyl (G) and syringyl (S) lignin, respectively (Rogers and Campbell 2004).
The first step in the lignin-specific branch of the phenylpropanoid pathway is catalysed by cinnamoyl-CoA reductase (CCR). This enzyme regulates the carbon flux towards lignin and is thus a viable target to alter lignin levels (Lacombe et al. 1997; Baucher et al. 1998). Genes encoding CCR have been studied in many species including the model plants Arabidopsis thaliana, Oryza sativa and Populus tremuloides (Costa et al. 2003; Li et al. 2003; Kawasaki et al. 2006). CCR1 genes have been found to be preferentially expressed in the stems of Panicum virgatum, A. thaliana, Medicago truncatula, Triticum aestivum, Lolium perenne and Zea mays (Pichon et al. 1998; Lauvergeat et al. 2001; Goujon et al. 2003; Larsen 2004; Ma and Tian 2005; Escamilla-Treviño et al. 2010; Tu et al. 2010; Zhou et al. 2010) and are thus thought to be involved in lignification. A reduction in the total lignin level and changes in monolignol composition were positively correlated with improved digestibility in the brown-midrib (bm) mutants of Z. mays as well as in transgenic plants in which caffeic acid 3-O-methyltransferase (COMT) was down-regulated (Baucher et al. 1998; Casler and Vogel 1999; Piquemal et al. 2002; Chen et al. 2004; Hisano et al. 2009; Tu et al. 2010; Tamasloukht et al. 2011). Down-regulation of CCR1 expression has been achieved in Nicotiana tabacum (Dauwe et al. 2007), Medicago sativa (Jackson et al. 2008), Solanum lycopersicon (Van der Rest et al. 2006) Z. mays (Park et al. 2012) and hybrid poplar (Populus tremula × Populus alba) (Leplé et al. 2007) as well as in the C3 forage, L. perenne, in which a decrease in total lignin was observed to correlate with improved digestibility (Tu et al. 2010).
Even moderate increases in digestibility have significant economic consequences; in L. perenne a 5–6 % increase in digestibility was estimated to increase summer milk production in southern Australia by up to 27 % (Smith et al. 1998). In this study we have isolated and characterised putative CCR1 cDNAs from P. dilatatum cv. Primo, a tetraploid sexually reproductive commercial cultivar. We describe the pattern of lignin deposition and CCR1 transcript levels during plant development and analyse the impact of down-regulating CCR1 on lignin composition and digestibility. Gene silencing was triggered by expression of a frame-shift mutant of a CCR gene, which was delivered separately to the selectable marker cassette. Both cassettes were delivered free of vector backbone.
Seeds of P. dilatatum cv. Primo, a tetraploid (2n = 4x = 40) sexually reproductive cultivar, kindly provided by Gustavo Schrauf, Facultad de Agronomía de la Universidad de Buenos Aires (FAUBA), were grown in glasshouses (21 °C, 14 h photoperiod/14 °C, 10 h dark period) or growth cabinets (21 °C, 14 h photoperiod/16 °C, 10 h dark period).
Isolation of putative cinnamoyl-CoA cDNAs from P. dilatatum
Reference sequences of CCR1 genes from Sorghum bicolor, Z. mays, P. virgatum and L. perenne were aligned and the consensus sequence was used to design primers to conserved regions. Sequences of all primers are provided as supporting information (Online Resource 1). Total RNA was extracted from 100 mg of ground tissue (stems, roots, leaf blades and inflorescences) from the final reproductive stage of P. dilatatum cv. Primo plants using the RNeasy® Plant Mini Kit (Qiagen, Hilden, Germany) according to manufacturer’s instructions. A cDNA library was prepared from pooled RNA using the SMART™ cDNA Synthesis kit (Clontech Laboratories, Mountain View, CA, USA). First strand cDNA was reverse transcribed using SMARTScribe™ Reverse Transcriptase and SMART IV™ oligonucleotides (Clontech Laboratories) and putative CCR genes were amplified from this template. Further transcripts were identified using the SMARTer™ RACE cDNA Amplification Kit (Clontech Laboratories). After re-amplification with proofreading polymerases, full-length coding sequences were cloned and sequenced using ABI Sanger Sequencing and Big Dye Terminator v3.1 (Life Technologies Corporation, Carlsbad, USA).
Southern hybridisation analysis
Genomic DNA was isolated from leaf tissue using a standard cetyltrimethylammonium bromide protocol (Doyle and Doyle 1987) and 10 μg was digested with one or more of the restriction enzymes HindIII, EcoRI and SacI in separate reactions and separated on a 0.8 % (w/v) agarose gel. Following electrophoresis, DNA was transferred to a Hybond N membrane (GE Healthcare, Little Chalfont, UK) using established protocols (Sambrook et al. 1989). A PdCCR-specific probe was generated using a PCR-based digoxigenin (DIG) Probe Synthesis Kit (Roche, Basel, Switzerland) according to the manufacturer’s instructions. Probes specific to the promoter of the polyubiquitin gene from Z. mays, present in the CCR-frameshift transgene cassette, and to the nptII selection gene were also made. Sequences of all primers are provided in Online Resource 1. Hybridisation with the PdCCR-specific probe was performed at 58 °C overnight and with the Z. mays polyubiquitin gene promoter and nptII gene probes at 55 °C overnight. A chemiluminescent detection protocol was used as per manufacturer’s instructions (DIG Luminescent Detection Kit, Roche).
The deduced amino acid sequences of the PdCCR transcripts identified in this study were aligned with previously derived CCR gene sequences as well as with sequences identified from publically available complete plant genomes using BLASTx and tBLASTn (cut-off of e−4). Reciprocal BLAST was performed against the A. thaliana and O. sativa genomes. Alignments were made using ClustalX (Larkin et al. 2007) and imported into Mesquite (Maddison and Maddison 2011) for refinement. A preliminary phylogenetic analysis showed that the clade containing the conserved NWYCY motif was monophyletic. Sequences from this clade were then subjected to rigorous analyses using the two most-closely related genes encoded in the genome of the bryophyte, Physcomitrella patens (from which no genes containing the conserved motif were identified) as an out-group. Ambiguously aligned characters were excluded in Mesquite, resulting in a matrix of 54 taxa and 313 characters. A maximum likelihood phylogeny was inferred using PhyML v3.0 (Guindon and Gascuel 2003) with the LG substitution model and eight categories of substitution rates. The alpha value and number of invariable sites were calculated from the data sets. Branch support was assessed using ML bootstrap analysis (PhyML with eight categories and 100 replications).
RNA was purified from plant tissue using the ZR Plant RNA MiniPrep™ Kit (Zymo Research, Irvine, CA) or the RNeasy Plant Mini Kit (Qiagen) according to manufacturer’s instructions. Expression of PdCCR during development of non-transgenic plants was analysed by quantitative reverse-transcriptase PCR (qRT-PCR) designed to amplify all CCR transcripts identified. Data was normalised using expression values of elongation factor-1 alpha (EF1α) as a reference gene (Silveira et al. 2009). Quantification was performed using SYBR Green Mastermix (Roche, Basel, Switzerland) with 200 nM of each primer for PdCCR amplification and with 300 nM of each primer for EF1α expression analysis. Cycling conditions were as follows: 95 °C for 10 min, 40 cycles of 95 °C for 30 s, and 60 °C (EF1α) or 63 °C (PdCCR) for 1 min, and 1 cycle of 95 °C for 1 min, 60 °C for 30 s and 95 °C for 30 s. Expression of PdCCR in transgenic plants was determined in the same way except that a set of primers spanning the coding and 3’ untranslated region was designed to amplify all CCR transcripts but to exclude amplification of transcript from the transgene cassette. Cycling conditions for this assay were as follows: 95 °C for 10 min, 40 cycles of 95 °C for 30 s, and 60 °C (EF1α) or 68 °C (PdCCR) for 1 min, and a hold of 95 °C for 1 min followed by a dissociation curve (60 °C to 95 °C). Sequences of all primers are provided in Online Resource 1. A tenfold dilution series of standard templates (linear double-stranded DNA) was prepared for absolute quantification. Standard error was calculated from three biological replicates. Amplification was performed on either an Mx3005P (Stratagene, Santa Clara, CA, USA) or a C1000 thermal cycler with the CFX96 real-time PCR detection system (Bio-Rad, Hercules, CA, USA). Results were analysed using the MxPro (Stratagene) or CFX Manager (Bio-Rad) software packages. Relative quantification was calculated according to the 2−∆∆Ct method (Livak and Schmittgen 2001).
Construction of expression cassettes
Expression cassettes consisting of the promoter and 5′ untranslated region (UTR) of the polyubiquitin (Ubi) gene from Z. mays (Toki et al. 1992), followed by the entire coding sequence of PdCCR1-1 with a frame-shift created by deleting the seventh base-pair downstream of the start codon and the 3′ UTR comprising transcriptional terminator and polyadenylation site from the fructosyltransferase 4 (FT4) gene from L. perenne were synthesised (GeneArt, Life Technologies, Regensberg, Germany). A plant selectable marker cassette consisting of the promoter and 5′ UTR from the actin (act1) gene from O. sativa (McElroy et al. 1990) followed by the neomycin phosphotransferase (npt2) gene was also synthesised. This cassette was terminated with the 3′ UTR, comprising transcriptional terminator and polyadenylation site, from the octopine synthase (oct) gene from Agrobacterium tumefaciens. Cassettes were liberated from the vector backbones by restriction digestion and separated from the plasmid DNA fragment using the Elutrap system (Whatman, Maidstone, UK) according to the manufacturer’s instructions.
Generation of transgenic P. dilatatum plants
A single genotype, Primo-11, was selected on the basis of observing shoot regeneration from embryogenic callus (EC) derived from mature seeds of P. dilatatum cv. Primo. This approach, including methods for surface sterilisation, callus induction from mature seed and vegetative in vitro tillers, shoot regeneration and maintenance of vegetative in vitro tillers, was adapted from Bajaj et al. (2006). Modifications to this method include a 15 min immersion of seeds in 50 % (v/v) sulphuric acid, the omission of endophyte control treatments, Murashige and Skoog (MS) media (Murashige and Skoog 1962) solidified with 0.7 % (w/v) agar (Sigma, St. Louis, MO, USA), the use of MS supplemented with 3 % (w/v) sucrose and 1 μM Kinetin (MSK) for shoot regeneration, the use of MS supplemented with 3 % (w/v) sucrose and 15 μM 6-benzylaminopurine (BA, Sigma, St. Louis, MO, USA) for maintenance medium and the use of MS supplemented with 3 % (w/v) sucrose and 22.6 μM 2,4-dichlorophenoxyacetic acid (2,4-D, Sigma, St. Louis, MO, USA) for callus induction medium.
Five to seven days prior to transformation EC were preconditioned by osmotic treatment on MS medium supplemented with 3 % sucrose, 64 g/L mannitol and 6 μM 2,4-D and incubated in the dark for 4 h at 24 ± 2 °C. EC were then bombarded with 0.6 μm gold particles coated with equal quantities of cassette DNA using the PDS 1000/He system (Bio-Rad) with a system pressure of 1,100 psi and a vacuum degree of 9.5 kPa (28 inches of mercury). Bombarded EC were kept in the dark for 16 h at 24 ± 2 °C before transfer to callus induction medium supplemented with 50 mg/L paromomycin as the selective agent. After 1 week, EC were transferred to regeneration medium supplemented with 50 mg/L paromomycin and incubated for 2 weeks at 24 ± 2 °C under a 16 h photoperiod at a photon flux density of 75 μM m−2 s−1. EC were subcultured every 2 weeks for 6 weeks on regeneration medium supplemented with 50 mg/L paromomycin. Putative transgenic plants with established roots were transferred to potting mix and grown in the glasshouse in conditions described above. Transgene was confirmed using qPCR to detect the endogenous gene EF1α, the selectable marker cassette and the PdCCR frameshift cassette. Sequences of all primers are provided as supporting information (Online Resource 1). Transgenic status was verified and copy number was determined by Southern hybridisation analysis as described above. Each transgenic line and two non-transgenic lines of the same genetic background, also regenerated in tissue-culture, were cloned into three biological replicates. Tissue samples of leaf blades and pseudostems of equivalent maturity were taken from each clone. Each sample was frozen in liquid nitrogen, ground and divided to provide material for expression and biochemical analyses. Each sample was analysed in triplicate to provide technical replicates.
Histochemical staining of lignin
The Mäule reagent specifically stains syringyl (S) lignin subunits red and guaiacyl (G) subunits brown (Iiyama and Wallis 1990; Lin and Dence 1992). Transverse sections of stems at different development stages were stained as previously described (Chen et al. 2002). Images were captured using a Leica MZ FLIII stereo fluorescence microscope with a Leica DFC300F colour camera (Leica Microsystems, Wetzlar, Germany).
Lignin content and composition analysis
Tissue samples were freeze-dried and homogenised to a fine powder using a mixer mill (MM400, Retsch Technology, Haan, Germany) at 25 Hz for two minutes. For isolation of cell walls, 100 mg of powdered leaf blade or stem tissue was sequentially extracted with hot water, ethanol and acetone. The remaining cell wall extract was used for determination of total lignin content and subunit composition analysis. The lignin content of leaf and stem tissues was quantified using the acetyl bromide soluble lignin method (Iiyama and Wallis 1990) with 6 mg of cell wall extract used per assay. Monolignol composition was determined with the thioacidolysis method (Rolando et al. 1992) using 8 mg of each cell wall extract per assay. Statistical analysis (Student t Test, P < 0.05) was carried out using Excel 2003 (Microsoft, Seattle, WA, USA).
Metabolite analysis of transgenic Paspalum dilatatum plants relative to control plants
Tissue samples were freeze-dried and homogenised to a fine powder. For the analysis of intermediate metabolites involved in monolignol synthesis, 50 mg of powdered leaf-blade tissue was extracted twice with one mL of 80 % methanol. The supernatants were combined and used directly for liquid chromatography-mass spectrometry (LC–MS) analysis. High-performance liquid chromatography (HPLC) separation was achieved using a 150 × 2.1 mm Agilent Eclipse XDB 1.9 μm C18 column fitted to an Agilent 1290 Infinity HPLC system (Agilent Technologies, Santa Clara, CA, USA). Metabolites were eluted from the column using a gradient mobile phase (containing water and acetonitrile) at a flow rate of 0.3 mL/min. The compounds were detected with a LTQ Orbitrap Velos mass spectrometer (Thermo Fisher Scientific, Waltham, MA, USA) with a heated electrospray ionisation source and a positive–negative switching scanning mode (both over the 80–2,000 m/z range). Standard compounds, namely p-coumaric acid, phenylalanine, ferulic acid, sinapic acid, and caffeic acid (all from Sigma-Aldrich) were analysed under the same conditions to identify metabolites of interest within the samples. Quantification of metabolites was performed using LCquan 2.0 software (Thermo Fisher Scientific) and statistical analysis (Student t Test, P < 0.05) was carried out using Excel 2003 (Microsoft).
Near-infrared reflectance spectroscopy (NIRS)
Vegetative herbage samples (cut 50 mm above the soil surface) were dried for 72 h at 55 °C and ground to a fine powder using a MM400 mixer mill (Retsch Technology) at 30 Hz for 2 min. Spectral data analysis was obtained and analysed and nutritive value estimated as described by Tu et al. (2010).
Isolation and characterisation of PdCCR1
The spatio-temporal pattern of PdCCR1 expression during plant development correlates with lignification
Three developmental stages of P. dilatatum cv. Primo, vegetative (V), early reproductive (R1) and late reproductive (R2), were selected for analysis of PdCCR1 expression, lignin deposition and composition. At V stage true stems have not yet formed and the plant is described as juvenile. Pseudostems are composed of the folded or rolled bases of leaves that have yet to emerge within a sheath. The reproductive stage is divided into early reproductive, R1, defined by the emergence of an inflorescence and late reproductive, R2, when the inflorescence is fully emerged and anthesis has commenced. At R1 and R2 stages almost all stems contain three internodes, basal (I1), middle (I2) and upper (I3), into which tissue was divided for analysis.
The spatio-temporal expression pattern of PdCCR1 expression through plant development was determined by qRT-PCR analysis of leaf blades and pseudostems sampled from the V stage and in the stem internodes and corresponding leaf from each internode at the R1 and R2 developmental stages using primers that detected all of the transcripts identified. The content of lignin as percentage of cell wall residue from the same tissues was quantified using an acetyl bromide soluble lignin assay.
Thioacidolysis of cell wall extracts to determine lignin subunit composition also showed that the content of G- and S-lignin increased as plants transitioned to the reproductive stage (Fig. 4B). In particular, the basal internodes of stems at the early reproductive stage (R1I1) contained five times as much S-lignin and twice as much G-lignin as pseudostems at V stage. This resulted in a change in S/G ratio from 0.19 to 0.35. Within reproductive stems the content of G- and S-lignin decreased with height. The S/G ratio was greatest in basal internodes (0.35 at R1 stage and 0.33 at R2 stage) and lowest in uppermost internodes (0.27 at R1 stage and 0.23 at R2 stage) (Fig. 4B). Conversely, no significant difference was observed in the lignin composition of leaf blades with the S/G ratio remaining between 0.20 and 0.26 in samples taken at all stages of development (Fig. 4B). The content of H-lignin remained low, typically 2–3 % of total lignin, in all tissues sampled (Fig. 4B).
Downregulation of PdCCR in transgenic P. dilatatum plants
Putative transgenic P. dilatatum plants, resistant to paromomycin were initially tested for the presence of transgenes by Southern hybridisation analysis (see Online Resource 2). Probes specific to the promoter of the polyubiquitin gene from Z. mays, designed to detect the PdCCR cassette, and to the nptII gene indicated that >5, 2 and 5 copies of the PdCCR cassette and >5, 1 and 6 copies of the nptII cassette were integrated in lines 76, 78 and 87 respectively (see Online Resource 2). In each line, the pattern of bands obtained with the two probes differed, indicating separate integrations of the PdCCR and nptII cassettes (see Online Resource 2), which suggests that the selectable marker may be removed by segregation in subsequent generations.
Although lignin content is lower in the vegetative stage than in reproductive stages,
Lignin content (% dry cell wall residues), composition (mg/g dry cell wall residues), and S/G ratio in leaf blades of transgenic lines and wild-type controls
15.07 ± 0.38
6.47 ± 0.79
1.69 ± 0.23
0.11 ± 0.02
13.94 ± 0.31
5.28 ± 0.63
1.70 ± 0.24
0.10 ± 0.02
15.39 ± 0.55
5.07* ± 0.17
1.57 ± 0.02
0.12 ± 0.00
12.28* ± 0.59
4.11 ± 0.45
1.63 ± 0.13
0.09 ± 0.01
Estimation of in vivo dry matter digestibility (IVVDMD) was performed using near-infrared reflectance spectroscopy (NIRS) as per Tu et al. (2010). Two transgenic lines showed a significant increase in IVVDMD in leaf blades (up to 4 %) in comparison to wild-type control lines, which correlated with a reduction in lignin (Online Resource 4).
The influence of lignin composition on cell wall digestibility has been studied in a number of forage species (Jung and Vogel 1986; Buxton and Russell 1988; Akin 1989; Jung and Deetz 1993; Grabber 2005). Increases in global mean temperature and expansion of the tropical zone mean that C4 grasses will become suitable forage crops in some regions that have historically been temperate. P. dilatatum, which is already grown for forage in sub-tropical regions, is a candidate species. In general, the lignin content (% dry cell wall) of C4 grasses is higher than that of C3 grasses (Jung and Vogel 1986). The lignin content of pseudostems from P. dilatatum plants at the early reproductive stage was found to be 5 % higher than that reported for equivalent tissues in the C3 grass L. perenne (Tu et al. 2010). Similarly, the basal internodes of stems at the late reproductive stage were found to have 5 % more lignin than equivalent tissue from F. arundinacea (Chen et al. 2002). Lignin composition in monocotyledons changes as plants transition from vegetative to reproductive developmental stages with S-lignin increasing and G-lignin decreasing upon flowering (Anterola and Lewis 2002; Chen et al. 2002; Guillaumie et al. 2008; Tu et al. 2010). In P. dilatatum, total lignin content increased through development with the percentage of H-lignin remaining constant but that of S- and G-lignin increasing five- and two-fold respectively.
Phylogenetic analysis showed that the putative CCR1 predicted proteins isolated from P. dilatatum in this study are closely related to CCR1 proteins involved in lignin deposition from other monocotyledonous plants, including those from wheat and L. perenne. The complete genomes of the monocotyledons Z. mays, O. sativa and B. distachyon all encode additional CCR proteins that resolved outside of the clade containing the CCR1 predicted proteins from P. dilatatum (Fig. 2). These include a protein annotated as CCR2 from T. aestivum (59805044) (Fig. 2). It is therefore likely that the P. dilatatum genome encodes CCR proteins additional to those described in this study.
Using primers designed to detect the three full length cDNAs isolated from P. dilatatum, it was found that transcripts of PdCCR1 were most abundant in tissues undergoing active lignification (R1, internodes two and three) and were less abundant in tissues such as R2 stage internodes and V stage leaf blades (Fig. 3) in which lignin had already accumulated. These observations are consistent with the idea that CCR1 is involved in constitutive lignification. This is similar to results reported for other species including L. perenne (Tu et al. 2010) and Leucaena leucocephala (Sirvastava et al. 2011).
Transgenic technologies have been widely used over the last decade to modify lignin content and composition in various model plants and crop species. Down-regulation of CCR in species such as N. tabacum (Piquemal et al. 1998; Ralph et al. 1998; Chabannes et al. 2001; O’Connell et al. 2002; Dauwe et al. 2007), S. lycopersicum (Van der Rest et al. 2006) M. sativa (Jackson et al. 2008), A. thaliana (Goujon et al. 2003) and L. perenne (Tu et al. 2010), has generally resulted in a reduction in lignin content. A reduction of lignin content, in particular large reductions of more than 30 %, have been associated with phenotypic abnormalities such as a reduction in plant size (Piquemal et al. 1998; Ralph et al. 1998; Chabannes et al. 2001; Goujon et al. 2003; Van der Rest et al. 2006; Dauwe et al. 2007; Prashant et al. 2011), delayed senescence (Mir Derikvand et al. 2008), delayed flowering (Prashant et al. 2011) and retarded seed development (Jones et al. 2001) or compromised pathogen defence (Prashant et al. 2011). These deleterious phenotypes infer that a very large reduction in lignin content is incompatible with normal growth and plant development. This suggests that there may be an optimal level to which lignin can be decreased for enhanced digestibility without an adverse effect on plant growth. P. dilatatum plants in which CCR was down-regulated showed no obvious deleterious developmental phenotypes compared to non-transgenic control plants when grown in standard glasshouse conditions. A moderate reduction in total lignin content (up to 20 %) was achieved in leaf blades. A decrease in levels of guaiacyl (G) subunits (up to 37 %) was observed in leaf blades, leading to an increase in the S/G ratio since syringyl (S) and hydroxyphenyl (H) subunit levels were not affected. These changes in composition are consistent with those observed in the ZmCCR1− mutant of Z. mays which showed only a 10 % reduction in lignin content while the S/G ratio increased (Tamasloukht et al. 2011).
In addition to changes in lignin composition, concentrations of p-coumaric acid, caffeic acid, ferulic acid and sinapic acid were observed to increase in the transgenic P. dilatatum lines. Similar results were observed in L. perenne transgenic lines (Tu et al. 2010) as well as in lignin-modified N. tabacum plants (Chabannes et al. 2001; Dauwe et al. 2007; Prashant et al. 2011), P. tremula × P. alba (Leplé et al. 2007) and A. thaliana (Goujon et al. 2003; Mir Derikvand et al. 2008). This increase indicates that metabolic intermediates have been re-directed into other pathways such as flavonoid biosynthesis, presumably as a result of reduced flux from coumaroyl-CoA, caffeoyl-CoA, and feruloyl-CoA to H- G-, and S- lignin (Leplé et al. 2007; Tu et al. 2010).
Our results suggest that PdCCR1 is involved in monolignol formation, most notably the production of G-lignin subunits. NIRS analysis estimated that a moderate reduction in total lignin and an increase in the S/G ratio correlate with an increase in digestibility. Similar results were also observed in the ZmCCR1−Z. mays mutant where cell wall digestibility improved by 24–28 % with only a 10 % reduction in lignin content (Tamasloukht et al. 2011).
The production of low-lignin C4 grasses with enhanced digestibility is desirable for the forage industry where they are considered more vigorous alternatives to temperate forage species and may increase milk production in the expanding tropical and warm temperate regions (Li et al. 2008; Seidel et al. 2008; Hisano et al. 2009). Engineering of C4 grasses with enhanced digestibility may also provide additional substrates for the cellulosic biofuel production industry. While further experiments are required to identify additional PdCCR gene family members, to investigate their roles and to isolate and characterise other enzymes in the lignin-biosynthesis pathway, it is clear that down-regulation of CCR1 is an effective strategy for the production of C4 forage grasses with decreased lignin content. Future studies will remove the selectable marker cassette by molecular breeding and assess the growth, fertility and agronomic performance of P. dilatatum germplasm with enhanced digestibility due to modification of lignin biosynthesis under field conditions.
We would like to thank Noel Cogan, Matthew Hayes and Daniel Isenegger for critical reading of the manuscript; Gustavo Schrauf from Facultad de Agronomía de la Universidad de Buenos Aires (FAUBA) for kind provision of P. dilatatum cv. Primo; Noel Cogan for advice with identification of CCR transcripts; Maiko Nakajima and Helen Huxley for purification of transgene cassette DNA; Roovini Weerasinghe for assistance with tissue culture; Pippa Kay for advice with quantitative real time PCR assays; Suzan Georges for advice on Southern hybridisation protocols; Carly Elliott for NIRS scanning and Larry Jewell, Alix Malthouse and Darren Callaway for growth and maintenance of all plants used in this study. This work was funded by the Dairy Futures Cooperative Research Centre, Australia. German Spangenberg and Aidyn Mouradov are inventors on US patent 2010/028766, ‘Modification of Lignin Biosynthesis Via Sense Suppression’.
- Bajaj S, Ran Y, Phillips J, Kularajathevan G, Pal S, Cohen D, Elborough K, Puthigae S (2006) A high throughput Agrobacterium tumefaciens-mediated transformation method for functional genomics of perennial ryegrass (Lolium perenne L.). Plant Cell Rep 25:651–659. doi:10.1007/s00299-005-0099-9 PubMedCrossRefGoogle Scholar
- Bernard-Vailh MA, Mign C, Cornu A, Maillot MP, Grenet E (1996) Effect of modification of the O-methyltransferase activity on cell wall composition, ultrastructure and degradability of transgenic tobacco. J Sci Food Agric 72:385–391. doi:10.1002/(SICI)1097-0010(199611)72:3<385:AID-JSFA664>3.0.CO;2-L CrossRefGoogle Scholar
- Chabannes M, Barakate A, Lapierre C, Marita JM, Ralph J, Pean M, Danoun S, Halpin C, Grima-Pettenati J, Boudet AM (2001) Strong decrease in lignin content without significant alteration of plant development is induced by simultaneous down-regulation of cinnamoyl CoA reductase (CCR) and cinnamyl alcohol dehydrogenase (CAD) in tobacco plants. Plant J 28:257–270. doi:10.1046/j.1365-313X.2001.01140.x PubMedCrossRefGoogle Scholar
- Chen L, Auh C, Chen F, Cheng X, Aljoe H, Dixon RA, Wang Z (2002) Lignin deposition and associated changes in anatomy, enzyme activity, gene expression, and ruminal degradability in stems of tall fescue at different developmental stages. J Agric Food Chem 50:5558–5565. doi:10.1021/jf020516x PubMedCrossRefGoogle Scholar
- Cook BG, Pengelly BC, Brown SD, Donnelly JL, Eagles DA, Franco MA, Hanson J, Mullen BF, Partridge IJ, Peters M, Schultze-Kraft R (2005) Tropical forages: an interactive selection tool (CSIRO, DPI&F(Qld), CIAT and ILRI, Brisbane) http://www.tropicalforages.info
- Costa MA, Collins RE, Anterola A, Cochrane F, Davin L, Lewis N (2003) An in silico assessment of gene function and organization of the phenylpropanoid pathway metabolomic networks in Arabidopsis thaliana and limitations thereof. Phytochemistry 64:1097–1112. doi:10.1016/S0031-9422(03)00517-X PubMedCrossRefGoogle Scholar
- Dauwe R, Morreel K, Goeminne G, Gielen B, Rohde A, Van Beeumen J, Ralph J, Boudet AM, Kopka J, Rochange SF, Halpin C, Messens E, Boerjan W (2007) Molecular phenotyping of lignin-modified tobacco reveals associated changes in cell-wall metabolism, primary metabolism, stress metabolism and photorespiration. Plant J 52:263–285. doi:10.1111/j.1365-313X.2007.03233.x PubMedCrossRefGoogle Scholar
- Doyle JJ, Doyle JL (1987) A rapid DNA isolation procedure for small quantities of fresh leaf tissue. Phytochem Bull 19:11–15Google Scholar
- Escamilla-Treviño L, Shen H, Uppalapati S, Ray T, Tang Y, Hernandez T, Yin Y, Xu Y, Dixon R (2010) Switchgrass (Panicum virgatum) possesses a divergent family of cinnamoyl CoA reductases with distinct biochemical properties. New Phytol 185:143–155. doi:10.1111/j.1469-8137.2009.03018.x PubMedCrossRefGoogle Scholar
- Guillaumie S, Goffner D, Barbier O, Martinant JP, Pichon M, Barrière Y (2008) Expression of cell wall related genes in basal and ear internodes of silking brown-midrib-3, caffeic acid O-methyltransferase (COMT) down-regulated and normal maize plants. BMC Plant Biol 8:71. doi:10.1186/1471-2229-8-71 PubMedCentralPubMedCrossRefGoogle Scholar
- Guo DJ, Chen F, Inoue K, Blount JW, Dixon RA (2001) Downregulation of caffeic acid 3-O-methyltransferase and caffeoyl CoA 3-O-methyltransferase in transgenic alfalfa: impacts on lignin structure and implications for the biosynthesis of G and S lignin. Plant Cell 13:73–88. doi:10.1105/tpc.13.1.73 PubMedCentralPubMedCrossRefGoogle Scholar
- Hutton EM, Nelson CJ (1968) Plant breeding and genetics. In: CSIRO TSotCL (ed) Some concepts and methods in sub-tropical pasture research. CSIRO, Brisbane, AustraliaGoogle Scholar
- Jung HG, Allen MS (1995) Characteristics of plant cell walls affecting intake and digestibility of forages by ruminants. J Animal Sci 73:2774–2790Google Scholar
- Jung HG, Deetz DA (1993) Cell wall lignification and degradability. In: Jung H, Buxton D, Hatfield R, Ralph J (eds) Forage cell wall structure and digestibility. Am Soc Agron, Madison, WI, pp 315–346Google Scholar
- Jung HG, Vogel KP (1986) Influence of lignin on digestibility of forage cell wall material. J Animal Sci 62:1703–1712Google Scholar
- Kawasaki T, Koita H, Nakatsubo T, K H, Wakabayashi K, Takahashi H, Umemura K, Yumezawa T, Shimamoto K (2006) Cinnamoyl-CoA reductase, a key enzyme in lignin biosynthesis, is an effector of small GTPase Rac in defense signaling in rice. Proc Natl Acad Sci USA 103:230–235. doi:10.1073/pnas.0509875103 PubMedCentralPubMedCrossRefGoogle Scholar
- Lacombe E, Simon H, Doorsselaere JV, Piquemal J, Goffner D, Poeydomenge O, Boudet A-M, Grima-Pettenati J (1997) Cinnamoyl CoA reductase, the first committed enzyme of the lignin branch biosynthetic pathway: cloning, expression and phylogenetic relationships. Plant J 11:429–441. doi:10.1046/j.1365-313X.1997.11030429.x PubMedCrossRefGoogle Scholar
- Lauvergeat V, Lacomme C, Lacombe E, Lasserre E, Roby D, Grima-Pettenati J (2001) Two cinnamoyl-CoA reductase (CCR) genes from Arabidopsis thaliana are differentially expressed during development and in response to infection with pathogenic bacteria. Phytochemistry 57:1187–1195. doi:10.1016/S0031-9422(01)00053-X PubMedCrossRefGoogle Scholar
- Leplé J-C, Dauwe R, Morreel K, Storme V, Lapierre C, Pollet B, Naumann A, Kang K-Y, Kim H, Ruel K, Lefebvre A, Joseleau J-P, Grima-Pettenati J, De Rycke R, Andersson-Gunneras S, Erban A, Fehrle I, Petit-Conil M, Kopka J, Polle A, Messens E, Sundberg B, Mansfield SD, Ralph J, Pilate G, Boerjan W (2007) Downregulation of cinnamoyl-Coenzyme A reductase in poplar: multiple-level phenotyping reveals effects on cell wall polymer metabolism and structure. Plant Cell 19:3669–3691. doi:10.1105/tpc.107.054148 PubMedCentralPubMedCrossRefGoogle Scholar
- Lin SY, Dence CW (1992) Methods in lignin chemistry. Springer, Berlin, GermanyGoogle Scholar
- Maddison WP and Maddison DR (2011) Mesquite: a modular system for evolutionary analysis. Version 2.75 http://mesquiteproject.org
- Mir Derikvand M, Sierra JB, Ruel K, Pollet B, Do CT, Thevenin J, Buffard D, Jouanin L, Lapierre C (2008) Redirection of the phenylpropanoid pathway to feruloyl malate in Arabidopsis mutants deficient for cinnamoyl-CoA reductase 1. Planta 227:943–956. doi:10.1007/s00425-007-0669-x PubMedCrossRefGoogle Scholar
- Park S-H, Mei C, Pauly M, Ong RG, Dale BE, Sabzikar, R, Fotoh H, Nguyen T, Sticklen M (2012) Downregulation of maize cinnamoyl-coenzyme A reductase via RNA interference technology causes brown midrib and improves ammonia fiber expansion-pretreated conversion into fermentable sugars for biofuels. Crop Sci 52:2687–2701Google Scholar
- Prashant S, Srilakshmi Sunita M, Pramod S, Ranadheer K, Gupta K, Anil Kumar S, Rao Karumanchi S, Rawal SK, Kavi Kishor PS (2011) Downregulation of Leucaena leucocephala cinnamoyl CoA reductase (LiCCR) gene induces significant changes in phenotype, soluble phenolic pools and lignin in transgenic tobacco. Plant Cell Rep 12:2215–2231. doi:10.1007/s00299-011-1127-6 CrossRefGoogle Scholar
- Ralph J, Hatfield RD, Piquemal J, Yahiaoui N, Pean M, Lapierre C, Boudet AM (1998) NMR characterization of altered lignins extracted from tobacco plants down-regulated for lignification enzymes cinnamylalcohol dehydrogenase and cinnamoyl-CoA reductase. Proc Natl Acad Sci USA 95:12803–12808. doi:10.1073/pnas.95.22.12803 PubMedCentralPubMedCrossRefGoogle Scholar
- Sambrook J, Fritsch EF, Maniatis T (1989) Molecular cloning: a laboratory manual. Cold Spring Harbor Laboratory, Cold Spring HarborGoogle Scholar
- Seidel DJ, Fu Q, Randel WJ, Reichler TJ (2008) Widening of the tropical belt in a changing climate. Nat Geosci 1:21–24Google Scholar
- Silveira ED, Alves-Ferreira M, Guimaraes LA, Rodriguez da Silva F, Campos Carneiro V (2009) Selection of reference genes for quantitative real-time PCR expression studies in the apomictic and sexual grass Brachiaria brizantha. BMC Plant Biol 9:84. doi:10.1186/1471-2229-9-84 PubMedCentralPubMedCrossRefGoogle Scholar
- Sirvastava S, Gupta K, Arha M, Vishwakarma K, Rawal SK, Kavi Kishor PB, Khan BM (2011) Expression analysis of cinnamoyl-CoA rreductase (CCR) gene in developing seedlings of Leucaena leucocephala: a pulp yielding tree species. Plant Physiol Biochem 49:138–145. doi:10.1016/j.plaphy.2010.11.001 CrossRefGoogle Scholar
- Smith KF, Simpson RJ, Oram RN, Lowe KF, Kelly KB, Evans PM, Humphreys MO (1998) Seasonal variation in the herbage yield and nutritive value of perennial ryegrass (Lolium perenne L.) cultivars with high or normal herbage water-soluble carbohydrate concentrations grown in three contrasting Australian dairy environments. Aust J Exp Agric 38:821–830. doi:10.1071/EA98064 CrossRefGoogle Scholar
- Tamasloukht B, Wong Quai Lam MS, Martinez Y, Tozo K, Barbier O, Jourda C, Jauneau A, Borderies G, Balzergue S, Renou JP, Huguet S, Martinant JP, Tatout C, Lapierre C, Barriere Y, Goffner D, Pichon M (2011) Characterization of a cinnamoyl-CoA reductase 1 (CCR1) mutant in maize: effects on lignification, fibre development, and global gene expression. J Exp Bot 62:3837–3848. doi:10.1093/jxb/err077 PubMedCentralPubMedCrossRefGoogle Scholar
- Tu Y, Rochfort S, Liu Z, Ran Y, Griffith M, Badenhorst P, Louie G, Bowman M, Smith K, Noel J, Mouradov A, Spangenberg G (2010) Functional analysis of Caffeic acid O-methyltransferase and cinnamoyl-CoA-reductase genes from perennial reygrass (Lolium perenne). Plant Cell 22:3357–3373. doi:10.1105/tpc.109.072827 PubMedCentralPubMedCrossRefGoogle Scholar
- Wilson JR (1993) Organisation of forage plant tissues. In: Jung H (ed) Forage cell wall structure and digestibility, American Society of Agronomy, Crop Science Society of America, Soil Science Society of America, Madison, WI, pp 1–32Google Scholar
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