Spatial gradients in cell wall composition and transcriptional profiles along elongating maize internodes
© Zhang et al.; licensee BioMed Central Ltd. 2014
Received: 16 August 2013
Accepted: 27 December 2013
Published: 14 January 2014
The elongating maize internode represents a useful system for following development of cell walls in vegetative cells in the Poaceae family. Elongating internodes can be divided into four developmental zones, namely the basal intercalary meristem, above which are found the elongation, transition and maturation zones. Cells in the basal meristem and elongation zones contain mainly primary walls, while secondary cell wall deposition accelerates in the transition zone and predominates in the maturation zone.
The major wall components cellulose, lignin and glucuronoarabinoxylan (GAX) increased without any abrupt changes across the elongation, transition and maturation zones, although GAX appeared to increase more between the elongation and transition zones. Microarray analyses show that transcript abundance of key glycosyl transferase genes known to be involved in wall synthesis or re-modelling did not match the increases in cellulose, GAX and lignin. Rather, transcript levels of many of these genes were low in the meristematic and elongation zones, quickly increased to maximal levels in the transition zone and lower sections of the maturation zone, and generally decreased in the upper maturation zone sections. Genes with transcript profiles showing this pattern included secondary cell wall CesA genes, GT43 genes, some β-expansins, UDP-Xylose synthase and UDP-Glucose pyrophosphorylase, some xyloglucan endotransglycosylases/hydrolases, genes involved in monolignol biosynthesis, and NAM and MYB transcription factor genes.
The data indicated that the enzymic products of genes involved in cell wall synthesis and modification remain active right along the maturation zone of elongating maize internodes, despite the fact that corresponding transcript levels peak earlier, near or in the transition zone.
KeywordsCell walls Cellulose Cereals Lignin Polysaccharides Transcription factors
Maize stover, which consists of the residual stalks and leaves of maize plants (Zea mays) that remain in the field after harvest, is becoming an increasingly important source of lignocellulosic biomass for second generation bioethanol production. Compositional analyses indicate that dried maize stover, which is composed almost completely of cell wall residues, contains high levels of cellulose, lignin and glucuronoarabinoxylans (GAX) . However, there is relatively little information available either on the distribution of these wall polymers in the mature plant or on their biosynthesis, re-modelling and degradation during normal growth and development. Similarly, little is known about the regulation of wall polysaccharide synthesis in vegetative tissues of maize.
Here, we have measured changes in cell wall composition along an elongating maize internode, which represents a useful model system for the examination of walls of the stalk at different stages of development. Thus, the basal region of the internode includes the intercalary meristem, above which is an elongation zone where cell expansion occurs and primary cell walls are deposited [2, 3]. Further up the internode is the transition zone, where cell elongation slows and secondary wall synthesis begins. At the upper or distal end of the internode is the maturation zone, where cells have stopped growing and secondary wall deposition predominates . The compositions of isolated walls in this developmental series have been monitored in 1 cm sections from the bottom of the internode. In parallel, microarray analyses have been used to define gene transcript profiles along the elongating internode and have enabled changes in wall composition to be reconciled with the transcriptional activities of genes involved in wall polysaccharide, protein and lignin synthesis, together with transcription factor genes that are known to regulate the expression of genes responsible for wall synthesis and re-modelling.
Cellulose accounts for about 50% of total dry matter in the mature stalk of maize and is synthesized by members of a family of cellulose synthase (CesA) enzymes, for which there are at least 12 genes in the maize genome . Cellulose is a linear polysaccharide of (1,4)-linked β-d-glucopyranosyl residues with a degree of polymerization from 2000 and up to 14,000, depending on the source [5, 6]. Cellulosic chains adopt extended ribbon-like conformations that allow the individual molecules to align into fibrillar aggregates that are stabilized by extensive intermolecular hydrogen bonding and van der Waals interactions, and exhibit high tensile strength. It has been variously suggested that each microfibril consists of 24 or 36 individual cellulose molecules [7, 8].
The other major cell wall polysaccharide of maize stover is glucuronoarabinoxylan (GAX) . The GAX components of walls in the grasses generally consist of a backbone of (1,4)-linked β-d-xylopyranosyl residues, some of which are substituted with single α-l-arabinofuranosyl residues at C(O)3 and to a lesser extent at C(O)2. The backbone β-d-xylopyranosyl residues can also be substituted at the C(O)3 position with α-d-glucuronopyranosyl residues or their 4-O-methyl ethers, or with short oligosaccharide chains. Hydroxycinnamic acid residues, in particular feruloyl residues, can be attached to the α-l-arabinofuranosyl residues [6, 9, 10].
Cell wall composition and properties are dynamic, insofar as they change during normal growth and development, and in response to abiotic and biotic stresses . In young, expanding cells the wall is relatively thin and is highly hydrated. The so-called primary cell is deposited during this developmental phase. The orientation of newly synthesized cellulosic microfibrils is transverse to the axis of the cell elongation , which constricts lateral expansion of the cell but allows turgor-driven cell expansion along the elongation axis. When cell expansion slows, the so-called secondary wall is formed, but it is likely that this transition occurs over a period of time rather than as an abrupt event. During the transition and maturation stages of cell development, cellulose, non-cellulosic polysaccharide and lignin concentrations of the wall increase and the structures of non-cellulosic polysaccharides can be altered to meet the changing functional requirements of the wall. These processes are of fundamental importance in allowing anisotropic growth in plant cells and, more specifically, for the elongation of maize internodes.
It has been estimated that approximately 1,200 genes encoding polysaccharide synthases, glycosyltransferases, glycosyl hydrolases and a range of ancillary and regulatory proteins are involved in plant cell wall biosynthesis, remodelling and degradation [13, 14]. Some information is also emerging on regulatory genes that participate in wall biology . In Arabidopsis, secondary wall-associated NAC (for NAM, ATAF1/2 and CUC2) domain protein 1 (SND1) regulate suites of target transcription factors, including SND2, SND3, MYB20, MYB42, MYB43, MYB52, MYB54, MYB69, MYB85, MYB103 and KNYT7 (a knotted1-like homeodomain protein) [16, 17]. More recently, interacting MYB75 and KNAT7 transcription factors have been shown to modulate secondary cell wall deposition both in stems and seed coat in Arabidopsis . In poplar (Populus trichocarpa), the wood-associated transcription factors (PtrWNDs) are the functional orthologs of Arabidopsis SND1 . They regulate a cascade of downstream transcription factors and control the biosynthesis of secondary walls. Pine MYB1 and MYB4 transcription factors and eucalyptus MYB2 regulate lignin biosynthesis by binding to the AC elements of promoters of lignin biosynthetic genes [20–23].
Regulation of wall synthesis and remodelling is also exerted at the protein level, where phosphorylation is an important mechanism for the regulation of enzymic activities. Phosphorylation of the AtCesA1 and AtCesA7 cellulose synthases has been reported in Arabidopsis [24, 25], where phosphorylation of AtCesA1, an enzyme that has been implicated in cellulose synthesis in primary walls, affects polar interaction with microtubules , while phosphorylation of AtCesA7, a secondary wall CesA, promotes the degradation of this enzyme.
In this study, the changes in cell wall polysaccharide compositions along an elongating maize internode have been compared with mRNA levels for genes encoding enzymes involved in cell wall metabolism, and a number of strong correlations have been observed in the various zones of the internode. For example, transcription of a several transcriptional factor and protein kinase genes is tightly correlated with the transcription of maize CesA10, CesA11 and CesA13 genes and with lignin metabolic genes.
The tenth internode of a maize stalk was divided into ten sections for analysis
When the 10th internode of a maize stalk was 10 cm in length, it was harvested and cut into 10 sections of approximately 1 cm each. At this time the internode was actively elongating and would normally elongate to about 15 cm within a couple of days . The basal Section S1 contained intercalary meristem cells. Sections S2 and S3 were the most actively elongating and are thus designated as the elongation zone here. Cell elongation persisted in Sections S4 and S5, but the elongation rate decreased, particularly in Section S5. We have designated Sections S4 and S5 as the transition zone. Cell elongation had almost or completely ceased in Sections S6 to S10 and substantial lignin deposition was observed. Sections S6–S10 were designated the maturation zone. Overall, the development and morphological appearance of the 10th internode of the maize stalk were as described previously by Morrison et al., Kende et al. and Bosch et al. .
Crystalline cellulose and lignin increase along the elongating internode
Substantial changes in wall polysaccharide composition and fine structure occur along the internode
The trend in the GAX contents of the walls was generally similar to that of cellulose, although GAX appeared to increase more between the elongation and transition zones. In the elongation zone, about 34% GAX was detected and this rose to about approx. 46% in the Section S8 of the maturation zone (Figure 2). Together, these two polysaccharides accounted for between 70 and 86% of the walls in the elongating maize internode. Other wall polysaccharides were also detected but were each generally less than 10% of the total. In each case these were more abundant in the elongation zone (Section S2 of Figure 2) and decreased to relatively low levels in the maturation zone (Section S8 of Figure 2). For example, the (1,3;1,4)-β-glucan concentration decreased from about approx. 12% to 4% from the base to the top of the internode (Figure 2).
Other minor components of the wall preparation, including pectic arabinan, arabinogalactan-proteins and galactomannans, also decreased from the base to the top of the internode (Figure 2). Overall, these developmental patterns of wall polysaccharides along the elongating maize internode were remarkably similar to those observed for developing barley coleoptiles, except that higher levels of pectic polysaccharides were detected in the walls of young barley coleoptiles .
Global gene transcription patterns vary significantly along the elongating internode
Of the 17,200 functionally annotated genes on the maize microarray, about 5% (930) encoded genes have been implicated in cell wall polysaccharide synthesis, lignin synthesis, or in metabolic pathways leading to the synthesis of wall constituents. When these genes were subjected to PCA analysis, they grouped into clusters that were similar to those observed for the entire gene set, although the S5 cluster merged with the S6-S10 cluster (Figure 3B). As expected, the data revealed spatial differences in the transcription patterns of genes associated with wall synthesis, re-modelling and degradation in meristematic, elongation and transition zones, but less pronounced differences between the transition and maturation zones (Figure 3B).
Differential expression of cell wall genes in an elongating maize internode
Number of genes changed by 2-fold or more (%)
% of differentially transcribed genes between any two sections
Transcription profiles of CesA genes show different patterns along the internode
The CesA genes from group 2 showed quite different transcription patterns. In each case transcript abundance increased from low levels in Section S1 to high levels in the transition zone Sections S3 and S4, before decreasing steadily in the maturation zone Sections S6-S10 (Figure 4B). These data are consistent with the apparent flattening out of crystalline levels after Sections S5 and S6 (Figure 1). Overall, levels of ZmCesA11 (Figure 4B) and ZmCesA12 (not shown) transcripts were low. Transcript profiles of these ZmCesA genes were checked by quantitative real-time PCR (QPCR) and showed good correspondence with the microarray data (Additional file 1: Figure S1).
Transcription profiles of cellulose synthase-like genes also show variable patterns
Two ZmCslF genes were represented on the microarray. Their transcript levels were generally low but relatively higher in Sections S3 and S4 (Figure 5 and Additional file 1: Figure S2). The maize genome is believed to have at least an additional five CslF and several CslH genes, but these were not represented on the microarray. Two ZmCslD genes were represented on the microarray, but their transcript levels were extremely low (data not shown).
Glycosyl transferase genes implicated in wall synthesis were differentially transcribed along the internodes
Genes involved in wall expansion and re-modelling are abundantly transcribed in all zones of the internode
Xyloglucan endotransglycosylases/hydrolases (XET) are believed to play a role in auxin-induced cell elongation [42, 45]. Their functions include modification of existing polysaccharide structures, in particular xyloglucans, and possibly the covalent cross-linking of different polysaccharides such as xyloglucans, cellulose and (1,3;1,4)-β-d-glucans [46–48]. Several putative XET genes were found on the microarray. The relative abundance of mRNA from the different XET genes varied widely, as did their transcription patterns (Figure 7B). In some cases, transcript levels were relatively high in the meristematic tissue of Section S1 and in other cases specific XET gene transcript levels remained high from the basal to the distal ends of the internode (Figure 7B).
Key sugar nucleotide interconversion gene transcripts peak in the transition zone
High transcription levels of polysaccharide endohydrolase genes were detected
Lignin pathway gene transcripts were high in the transition and lower maturation zones
A few other lignin-related genes showed increased transcription along the internode sections and remained high in the maturation zone (Additional file 1: Figure S3). These included two CCR genes (Q84JG9, Q24563), three peroxidase genes (Q43416, Q5I3F1, Q9ZTF7) and ferulate 5-hydroxylase (F5H, Q109F2). One of the lignin metabolism genes (Q8W2X2) had relatively high transcript levels in Sections S1 and S2 (Additional file 1: Figure S3), but low transcript levels in the transition and maturation zones.
Transcription factor gene transcripts were detected
The MYB transcription factors have diverse functions in the regulation of gene transcription and a few of this class are believed to be targets of the NAC-domain transcription factors [52–54]. More than 100 putative MYB transcription factors annotations were found on the microarray. Eleven of these had very high transcript levels in the elongation internode (Figure 11B). The mRNA levels of 4 MYB genes (Q2A702, A2X8K7, Q8S415 and Q4L214) were low in Section S1, increased in Section S2, peaked at either Section S3 or Section S4, decreased in Section S5 and remained low in Sections S6 to S10 (Figure 11). Transcription activity of the MYB gene (Q7XC51) was also low in Section S1, increased in Section S2, peaked at Section S4, decreased in Section S5 and S6, and peaked again in Section S7. The transcript level of this MYB gene was most abundant among all MYB genes (Figure 11B).
When cell wall compositions were determined in ten sections of the elongating tenth internode of V16 stage maize plants, it was apparent that crystalline cellulose levels increased from about 20% by weight in the lower meristematic regions of the internode to over 40% in the upper S9 section of the maturation zone, although the rate of increase decreased after Section S6 (Figure 1). The cellulose contents estimated from methylation-based linkage analyses as (1,4)-glucosyl residues [31, 32] were generally higher than the values for crystalline cellulose (compare Figure 1 and Figure 2) and would include both crystalline and non-crystalline cellulose (cf. ), but the proportions of crystalline cellulose were decreased in the lower, younger regions of the internode. Thus, approximately 70% crystalline cellulose was measured in Section S2 and 95% in Section S8. Lignin also showed a similar steady rate of increase in the internodes, from about 15% by weight in the lower sections to about 30% by weight in the upper regions of the maturation zone. In neither case were any abrupt changes observed in cellulose or lignin concentrations as the developmental stage of the internode cells passed from meristematic tissues, through the elongation zone, transition zone and the maturation zone. In absolute terms, Scobbie et al. showed that total cell wall concentrations were higher in the maturation zone than in lower sections of the internode.
The major non-cellulosic polysaccharide in wall preparations from the ten internode sections was GAX, which was estimated from the linkages analyses based on previously published structures of these polysaccharides . Levels of GAX in the isolated walls were about 32% in the elongation zone Section S1, but increased sharply to about 45-50% in the transition and maturation zones (Figure 2). An important characteristic of the cell wall is that the plant can adjust the physicochemical properties of constituent polysaccharides and hence their function in the wall. For example, in the case of GAX, the degree of substitution of the (1,4)-β-xylan backbone can be altered. A lower degree of substitution will enable chains to form intermolecular hydrogen bonding with the (1,4)-β-xylan backbone of other GAX molecules, or with cellulose . Here, the degree of substitution of the xylan backbone with arabinosyl residues decreased markedly along the internode, but in particular between the elongation zone and the transition zones. The average Xyl:Ara ratios in the GAX, taken from three biological replicates, was 1.6:1 for Section S2, 6.6:1 for Section S4, 8.2:1 for Section S6 and 7.5:1 for Section S8 (data not shown). From these values, one would predict that the solubility of the GAX would decrease dramatically along the internode and that the ability of the GAX to interact with other polysaccharides through molecular alignment and intermolecular hydrogen bonding, would greatly increase, especially between the elongation and transition zones. From the overall colorimetric analyses of uronic acids in the sections, it was possible to estimate that the degree of substitution of the xylan backbone of the GAX with GlcA residues was about 30% in Section S2 of the elongation zone, but this decreased to about 10% in the transition zone and maturation zone Sections S4, S6 and S8 (data not shown). The overall uronic acid levels of 3.5% to 5% by weight of the internode were comparable with the values of 4% reported for barley husk . These uronic acid contents are deduced to be primarily GlcA and hence present on the GAXs as terminal residues, because carboxyl reduction/methylation analyses of the elongation zone (data not shown) showed negligible levels of either terminal- or 4-GalA residues, which suggested that only low levels of pectic galacturonans/RG1 were present, consistent with the virtual absence of Rha residues in the sugar analyses.
Minor polysaccharides of the walls included xyloglucans, (1,3;1,4)-β-glucans, galactomannans, arabinans and type II arabinogalactans. These showed similar changes along the elongating internode; in each case their levels decreased steadily from the lower to the upper regions of the internode, again without any abrupt changes between the different developmental stages represented by the elongation, transition and maturation zone sections (Figure 2).
Attempts were subsequently made to reconcile the changes in compositions of cell walls described above with changes in gene expression, as measured by transcript abundance in the ten sections of the elongating internode. In undertaking these comparisons, it is important to note that transcript abundance will not necessarily be directly related to levels of the encoded enzymes and, similarly, will not always be proportional to the levels of polysaccharide products of the synthase enzymes. Nevertheless, many consistent trends were observed between transcript levels and cell wall composition. Microarray techniques were applied to this question and when both total gene transcripts and the levels of transcripts of genes that can be linked with cell wall metabolism were analysed, easily discerned differences in transcript profiles between the internode sections became apparent. Principal component analyses (PCA) highlighted these differences (Figure 3A cf. Figure 3B) and we conclude from these data that it is necessary to divide the elongating maize internode into sections to obtain a more complete understanding of changes in gene transcription at different developmental stages. This approach may be contrasted with that of Bosch et al. who compared elongating and non-elongating whole maize internodes for their microarray experiments.
Cellulose biosynthesis is catalysed by at least two groups of CesA enzymes. One group is believed to be responsible for cellulose synthesis in the primary wall and the other for secondary wall cellulose synthesis . In the maize genome, 12 CesA genes have been identified . Transcripts of CesA10, CesA11 and CesA12 genes are abundant in vascular bundles and these have been implicated in secondary wall cellulose synthesis . The maize genomic DNA sequence has revealed another secondary wall CesA gene, which had a similar sequence with CesA12 gene and is designated CesA13.
Transcript levels for the ZmCesA gene family were determined along the elongating tenth internode and particular attention was paid to transcript levels of ZmCesA genes that have previously been implicated in cellulose synthesis either in primary or secondary walls . One might expect that transcripts for primary wall CesA genes would have been highest in the meristematic and elongation regions of the internode and to have subsequently decreased in the transition and maturation zones, but this was not observed. Of the ZmCesA genes representative of those proposed to be involved in primary wall cellulose biosynthesis, most showed relative low levels of transcript right along the internode (Figure 4A). The notable exception here was the ZmCesA7 gene, for which relatively high transcript levels were detected in the transition and maturation zones of the internode (Figure 4A). At this stage we are unable to explain the transcript pattern for the ZmCesA7 gene.
Transcript levels for the secondary cell wall ZmCesA genes were relatively low in the meristematic tissues and in the elongation zone, as expected, but increased quickly in the upper elongation zone and the transition zone to show a quite distinct peak in the transition zone, whereafter they steadily decreased (Figure 4B). Similarly, transcript levels for genes encoding enzymes involved in monolignol biosynthesis and other steps in lignin biosynthesis  were low in the lower sections of the internode, as expected, but increased to a marked peak in the transition zone before steadily decreasing in the maturation zone (Figure 10). These characteristic transcription patterns for the cellulose synthase and lignin synthesis genes must be reconciled with the steady increases of both cellulose and lignin from the lower elongation zone to the upper maturation zone of the internode (Figure 1). One explanation would be that the CesA enzymes and those involved in lignin synthesis are relatively stable and, once synthesised, can continue to generate cellulose and lignin over several days in the maturation zone. Another possibility is that a pool of lignin monomers is generated and that their polymerization into lignin continues over several days. In the case of cellulose, the formation of crystalline forms might lag behind the synthesis of the nascent cellulose chains, although the decrease in secondary wall CesA mRNA levels in the maturation zone (Figure 10) matches the slower rate of increase in cellulose after Sections S5 and S6 (Figure 1). Whatever the explanation, it is clear that the peaks and troughs of transcript levels observed here in the different regions of the internode are ‘flattened out’ to allow a steady increase in crystalline cellulose and lignin from the bottom to the top of the elongating internode (Figure 1).
The developmental patterns of transcripts of genes that are believed to mediate GAX synthesis were somewhat harder to interpret, mainly because our current understanding of heteroxylan synthesis is incomplete. Nevertheless, a number of genes have been shown to be involved. Members of the GT43 and GT47 families of glycosyl transferases are thought to be involved in the elongation of the xylan backbone [36, 38, 41, 57, 58], GT8 enzymes have been shown to be involved in glucuronosyl substitution of the xylan chain [39, 59, 60] and GT61 enzymes are likely to be arabinosyl or xylosyl transferases [61, 62]. The most abundant transcripts from these groups of genes were those encoding GT43 enzymes, which showed developmental patterns (Figure 6A) that were remarkably similar to those of the secondary cell wall cellulose synthases (Figure 4B). In both cases transcripts peaked in the transition zone and in the lower maturation zone. These observation are consistent with suggestions that the GT43 enzymes mediate (1,4)-β-xylan chain elongation. However, levels of gene transcripts for the enzymes believed to be involved in xylan backbone substitution, namely the GT8 and GT61 enzymes, remained low along the entire length of the internode (Figure 6B).
Transcript levels for the UXS gene, which encodes an enzyme that is central to the synthesis of the important GAX sugar donor substrates, namely UDP-Xyl and UDP-Ara, followed a similar pattern to the GT43 gene and the secondary wall CesA genes (Figure 8), while the UGPP gene that commits carbon to sugar-nucleotide synthesis more generally, was transcribed at high levels right along the internode, but again with a peak in the transition zone (Figure 8).
Of the genes that have been implicated in the biosynthesis of the minor non-cellulosic wall polysaccharides, CslE3 gene transcripts were the most abundant; the functions of CslE enzymes have not been defined. Surprisingly high levels of CslA1 transcripts were detected in the meristematic tissues of Section S1, but these decreased quickly in the elongation zone before rising again during maturation (Figure 5). As noted earlier, CslA genes are believed to be involved in mannan and glucomannan synthesis [33, 34], but there is only about 3% (w/w) mannan in the walls in the elongation zone, and this decreases to and remains at very low levels thereafter (Figure 2 and our unpublished data). It has been observed elsewhere that mannan levels and CslA transcripts are relatively high at the early stages of development of barley endosperm  and barley coleoptiles , but the data suggest that mannans might be more important in the early stages of wall deposition in very young tissues.
During the elongation phase of anisotropic cell growth, a number of enzymes and proteins, including expansins and xyloglucan endotransglycosylases (XETs), are believed to mediate in the wall loosening process that is considered essential for cell expansion to occur . Transcripts of genes encoding both classes of proteins were detected at high levels along the maize internode (Figure 7). Many of the expansin gene transcripts preceded the secondary wall CesA and lignin-associated genes (Figure 7A cf. Figure 4A and Figure 10), with peak levels in the elongation zone. This is consistent with the expansion of cells in those zones of the internode. In contrast, the patterns of XET transcript development were highly variable and could not be easily linked with changes in internode developmental stages or wall composition (Figure 7B). The XET gene families in plants are generally large  and the enzymes have been implicated not only in xyloglucans modification, but also in the modification or covalent cross-linking of cellulose and various non-cellulosic wall polysaccharides [46–48, 65]. Participation in the re-modelling of a range of wall polysaccharides would be consistent with the highly variable transcript profiles observed in the elongating maize internode (Figure 7B).
Other genes that have been implicated in wall re-modelling, but also in turnover and degradation, include polysaccharide hydrolases. For example, high levels of transcripts for a β-glucan exohydrolase were observed, with maximal levels in the transition zone (Figure 9A). The β-glucan exohydrolase is a non-specific exo-acting enzyme that is capable of hydrolysing a wide range of oligoglucosides and might be required to completely degrade various β-glucans to their constituent sugars . In contrast, one of the (1,3;1,4)-β-glucanase genes decreased steadily from the lower internode regions to the upper maturation zone (Figure 9B). This paralleled the decreases in (1,3;1,4)-β-glucan concentration in the wall along the internode (Figure 2). However, another (1,3;1,4)-β-glucanase gene was transcribed in the transition zone and lower maturation zone (Figure 9B), when the levels of (1,3;1,4)-β-glucan were very low indeed. Transcripts of several genes encoding (1,3)-β-glucanases were also detected (Figure 9A), but these enzymes are encoded by a very large gene family and perform a wide range of functions in plants , consistent with the range of developmental patterns seen in the elongating maize internode (Figure 9A).
It is noteworthy that the same five β-expansin genes and one of the XET genes (Q5JZX2) observed here also play a role in gravitation-induced cell elongation in the maize pulvini . The transcript levels of these genes increase substantially in the lower pulvini, where cell elongation is induced by gravitational stress . The (1,3;1,4)-β-glucanase and the β-1,3-glucananase genes are also showed to be involved in gravitation-induced cell elongation in the lower region of maize pulvini . Thus, it appears that the genes identified in the present study through their high transcript levels in the normal growth and development of elongating maize internodes are also transcribed in response to gravitational stress.
Correlation analysis of cell wall genes in the elongating maize internode
Cell wall metabolism
Glycosyltransferase (Q50HU5, GT43 family)
Glycosyltransferase (Q50HW1, GT43 family)
(1,3;1,4)-β-glucanase (Q7DLM1, GT17)
Caffeoyl CoA 3-O-methyltransferase (Q7XYW7)
Caffeoyl CoA 3-O-methyltransferase (Q6VWH0)
Cinnamyl alcohol dehydrogenase (O24562)
4-coumarate coenzyme A ligase (Q6Q297)
Peroxidase P7X (Q9ZTS7)
Carboxylate oxidase (Q75IP9)
Transcription factor and protein kinases
Nucellin-like aspartic protease (Q5Z6M6)
Putative blue copper protein (Q6Z7U7)
Cdc protein kinase-like (Q653F8)
LEM3 (Ligand-effect modulator 3)-like (Q653D8)
POT family protein (Q2R726)
Protein kinase (Q2RBK1)
Putative NEP1-interacting protein (Q6Z2U9)
Serine/threonine-protein kinase SAPK3 (Q75V63)
High correlations were also observed between the secondary wall ZmCesA gene transcripts and various protein kinases (Table 2). Although the roles of these kinases in the regulation of cellulose synthesis have not been examined further here, it seems likely from other studies that phosphorylation or de-phosphorylation of CesA enzymes affects their activities. For example, phosphorylation of the Arabidopsis AtCesA7 protein, a subunit of the secondary wall CesA complex, targets this protein for a degradation, while mutation of the phosphorylation sites of the Arabidopsis AtCesA1 enzyme, which is involved in primary wall cellulose synthesis, affects polar interactions between the CesA complex and microtubules [24, 25]. In the elongating maize internode, transcription of two protein kinases (Q653F8 and Q75V63) is highly correlated with transcription of secondary wall CesA genes (Table 2).
Analyses of wall compositions and transcript profiles in 1 cm sections of the elongating 10th internode of maize plants revealed several unexpected developmental patterns. Firstly, the three major cell wall components, cellulose, GAX and lignin, increased relatively steadily without any abrupt changes between the elongation, transition and maturation zones of the elongating internode. Secondly however, transcript profiles of genes known to be involved in the synthesis or re-modelling of these major wall components did not match the steady increases in cellulose, GAX and lignin mentioned above. Instead, transcript levels of many of these genes were low in the meristematic and elongation zones, quickly increased to maximal levels in the transition zone and lower sections of the maturation zone, and generally decreased in the upper maturation zone sections towards the top of the internode. Genes with transcript profiles showing this pattern included secondary cell wall CesA genes, GT43 genes, some β-expansins, UXS and UGPP, cellulase, most of the genes in metabolic pathways leading to the synthesis of monolignols, and NAM and MYB transcription factor genes. The fact that transcription of many of these genes decreased along the maturation zone, where the levels of cellulose, GAX and lignin continued to increase, suggested that the enzymic products of the genes remained active right along the maturation zone, despite the fact that the corresponding transcript levels had declined. Furthermore, the analyses enabled us to identify transcription factors and protein kinases that are potentially involved in the regulation of cell wall synthesis and the functions of some of these genes are currently under investigation.
Maize plants (O9B) were grown in a glasshouse at 17/27°C under natural light conditions. An elongating internode (about 10 cm in length) from the V16 developmental stage of maize  plants was harvested, cut into 10 sections and frozen immediately in liquid nitrogen for cell wall polysaccharide and mRNA preparation.
Cell wall preparation and analysis
Cell wall polysaccharides were determined as described previously . Maize stalk sections were ground under liquid nitrogen, exhaustively extracted with 80% v/v ethanol and the residue (AIR) thoroughly de-starched with pancreatic α-amylase . The ethanol-insoluble residues (de-starched AIR) were dried by solvent exchange with methanol and acetone, and stored in a vacuum desiccator with dried silica gel. Crystalline cellulose was determined by the acetic acid/nitric acid method of Updegraff , with modifications as described in Pettolino et al.. The procedure was accurate to approximately 3%. Lignin was determined colorimetrically by the acetyl bromide method as described by Hatfield et al. with the following modifications. Approximately 2 mg cell wall material (in duplicate) was hydrolysed with 0.5 mL 25% acetyl bromide in acetic acid (v/v) for 2.75 h at 70ºC, followed by the addition of 4.4 mL of a premixed solution of 10 mL 2 M NaOH with 12 mL acetic acid, made up to 10 mL by weight. Absorbance was measured at 280 nm and lignin calculated based on an extinction coefficient of 20 gL-1cm-1.
Monosaccharide linkage analysis was performed in duplicate by methylation with methyl iodide in sodium hydroxide and DMSO as described by Ciucanu and Kerek  followed by hydrolysis, reduction and acetylation and data calculated as mol% of total AIR, as previously described [31, 32]. Monosaccharide linkages (mol%) and relative polysaccharide proportions were deduced from the partially methylated alditol acetates that were separated and analysed by GC-MS as previously described [31, 32]. Using these procedures and the known structures of wall constituents, it is possible to assign individual partially methylated alditol acetate derivatives, or portions thereof, to different wall polysaccharides. For example, 4-linked glucosyl residues can be assigned to xyloglucan, cellulose and/or (1,3;1,4)-β-glucan, while galactosyl residues might be assigned to pectins, arabinogalactan-proteins, xyloglucans, etc. A complete description of the formulae used for these calculations is provided in Pettolino et al..
Uronic acids were assayed according to Filisetti-Cozzi and Carpita  with some modifications. Briefly, d-glucuronic acid was used as the calibration standard (1 mg/mL). Sample tubes were prepared by the addition of 0.4 mL water in 10 mL tubes at 4°C, and 80 μL 4 M sulfamic acid-potassium sulfamate (pH 1.6) and 2.4 mL 75 mM sodium tetraborate in concentrated H2SO4 were added. In a separate tube, approximately 2 mg sample was weighed and hydrolysed in 200 μL 75 mM sodium tetraborate in concentrated H2SO4. A 20 μL aliquot of the hydrolysed sample was added to the sample tubes containing sulfamic acid-potassium sulfamate and sodium tetraborate. All tubes were pulsed in a centrifuge and heated in a water bath to 90°C for 20 minutes, whilst ensuring the water level did not exceed that within the tubes by more than 1 cm. Tubes were cooled on ice and absorbance was measured at 525 nm. This was followed by the addition of 80 μL 0.15% m-hydroxybiphenyl in 0.5% sodium hydroxide. Tubes were mixed and allowed to rest for 10 min to allow colour to develop, before absorbance was measured at 525 nm.
Transcript profiling by microarrays
Microarray analyses were conducted as described previously . Maize internode sections were ground under liquid nitrogen and total RNA extracted with the TRIZOL reagent (Invitrogen, Sydney) according to the manufacturer’s instructions. Polyadenylated mRNA was purified using the Illustra mRNA Purification Kit (GE Biosciences). Sample quality and RNA concentration were assessed using an Agilent Bioanalyzer. The mRNA was reverse-transcribed into double-stranded cDNA, which was labelled with Cy3 or Cy5 fluorescent dye, using the Agilent Low RNA Linear Amp kit. Biological replicates were labelled alternately using Cy3 or Cy5 to guard against dye-bias. The cDNA was hybridized to Agilent 4 × 44 k maize gene microarrays  and the microarrays were washed according to Agilent standard protocols. The microarray chips were scanned with an Agilent G2505B DNA Microarray Scanner at two laser power settings (100% and 10%). The images were inspected visually for image artefacts, and feature intensities were extracted, filtered and normalized with Agilent Feature Extraction Software (v 9.5.1). The data were normalized using quantile normalization (BOLSTAD http://www.ncbi.nlm.nih.gov/pubmed/12538238). The normalized data were used to compare expression levels of genes related to cell wall compositions.
Quantitative RT-PCR analysis of maize cell wall genes
Transcription analysis of maize cell wall genes was carried by real time PCR (Q-PCR) according to Burton et al.. The same batch of RNA used for the microarray analysis was used for the synthesis of cDNA. The primer sequences used for Q-PCR are listed in Additional file 1: Table S2.
This work was supported by grants from the Australian Research Council. We thank Cherie Walsh, Natalie Kibble and Jessica Smith for their expert technical assistance.
- Pordesimo L, Hames B, Sokhansanj S, Edens W: Variation in corn stover composition and energy content with crop maturity. Biomass Bioenergy. 2005, 28 (4): 366-374. 10.1016/j.biombioe.2004.09.003.View ArticleGoogle Scholar
- Kende H, van der Knaap E, Cho H-T: Deepwater rice: a model plant to study stem elongation. Plant Physiol. 1998, 118 (4): 1105-1110. 10.1104/pp.118.4.1105.PubMed CentralView ArticlePubMedGoogle Scholar
- Scobbie L, Russell W, Provan GJ, Chesson A: The newly extended maize internode: A model for the study of secondary cell wall formation and consequences for digestibility. J Sci Food Agric. 1993, 61 (2): 217-225. 10.1002/jsfa.2740610213.View ArticleGoogle Scholar
- Appenzeller L, Doblin M, Barreiro R, Wang HY, Niu XM, Kollipara K, Carrigan L, Tomes D, Chapman M, Dhugga KS: Cellulose synthesis in maize: isolation and expression analysis of the cellulose synthase (CesA) gene family. Cellulose. 2004, 11 (3–4): 287-299.View ArticleGoogle Scholar
- Bacic A, Harris PJ, Stone BA: Structure and function of plant cell walls. The Biochemistry of Plants. Edited by Preiss J. San Diego: Academic Press; 1988:297–371.View ArticleGoogle Scholar
- Fincher GB, Stone BA: Chemistry of nonstarch polysaccharides. InEncyclopedia of Grain Science. Edited by Wrigley C, Corke H, Walker CE.Oxford: Elsevier; 2004.Google Scholar
- Doblin MS, Kurek I, Jacob-Wilk D, Delmer DP: Cellulose biosynthesis in plants: from genes to rosettes. Plant Cell Physiol. 2002, 43 (12): 1407-1420. 10.1093/pcp/pcf164.View ArticlePubMedGoogle Scholar
- Thomas LH, Forsyth VT, Šturcová A, Kennedy CJ, May RP, Altaner CM, Apperley DC, Wess TJ, Jarvis MC: Structure of cellulose microfibrils in primary cell walls from collenchyma. Plant Physiol. 2013, 161 (1): 465-476. 10.1104/pp.112.206359.PubMed CentralView ArticlePubMedGoogle Scholar
- Carpita NC: Update on mechanisms of plant cell wall biosynthesis: how plants make cellulose and other (1 → 4)-β-d-Glycans. Plant Physiol. 2011, 155 (1): 171-184. 10.1104/pp.110.163360.PubMed CentralView ArticlePubMedGoogle Scholar
- Fincher GB: Revolutionary times in our understanding of cell wall biosynthesis and remodeling in the grasses. Plant physiology. 2009, 149 (1): 27-37. 10.1104/pp.108.130096.PubMed CentralView ArticlePubMedGoogle Scholar
- Doblin MS, Pettolino F, Bacic A: Evans Review: Plant cell walls: the skeleton of the plant world. Funct Plant Biol. 2010, 37 (5): 357-381. 10.1071/FP09279.View ArticleGoogle Scholar
- Anderson CT, Carroll A, Akhmetova L, Somerville C: Real-time imaging of cellulose reorientation during cell wall expansion in arabidopsis roots. Plant Physiol. 2010, 152 (2): 787-796. 10.1104/pp.109.150128.PubMed CentralView ArticlePubMedGoogle Scholar
- Burton RA, Ma G, Baumann U, Harvey AJ, Shirley NJ, Taylor J, Pettolino F, Bacic A, Beatty M, Simmons CR, et al: A customized gene expression microarray reveals that the brittle stem phenotype fs2 of barley is attributable to a retroelement in the HvCesA4 cellulose synthase gene. Plant Physiol. 2010, 153 (4): 1716-1728. 10.1104/pp.110.158329.PubMed CentralView ArticlePubMedGoogle Scholar
- Somerville C, Bauer S, Brininstool G, Facette M, Hamann T, Milne J, Osborne E, Paredez A, Persson S, Raab T, et al: Toward a systems approach to understanding plant cell walls. Science. 2004, 306 (5705): 2206-2211. 10.1126/science.1102765.View ArticlePubMedGoogle Scholar
- Carpita NC: Progress in the biological synthesis of the plant cell wall: new ideas for improving biomass for bioenergy. Curr Opin Biotechnol. 2012, 23 (3): 330-337. 10.1016/j.copbio.2011.12.003.View ArticlePubMedGoogle Scholar
- Olsen AN, Ernst HA, Lo Leggio L, Skriver K: NAC transcription factors: structurally distinct, functionally diverse. Trends Plant Sci. 2005, 10 (2): 79-87. 10.1016/j.tplants.2004.12.010.View ArticlePubMedGoogle Scholar
- Zhong RQ, Lee CH, Zhou JL, McCarthy RL, Ye ZH: A battery of transcription factors involved in the regulation of secondary cell wall biosynthesis in arabidopsis. Plant Cell. 2008, 20 (10): 2763-2782. 10.1105/tpc.108.061325.PubMed CentralView ArticlePubMedGoogle Scholar
- Bhargava A, Ahad A, Wang S, Mansfield SD, Haughn GW, Douglas CJ, Ellis BE: The interacting MYB75 and KNAT7 transcription factors modulate secondary cell wall deposition both in stems and seed coat in Arabidopsis. Planta. 2013, 237 (5): 1199-1211. 10.1007/s00425-012-1821-9.View ArticlePubMedGoogle Scholar
- Zhong R, Ye ZH: The poplar PtrWNDs are transcriptional activators of secondary cell wall biosynthesis. Plant Signal Behav. 2010, 5 (4): 469-472. 10.4161/psb.5.4.11400.PubMed CentralView ArticlePubMedGoogle Scholar
- Goicoechea M, Lacombe E, Legay S, Mihaljevic S, Rech P, Jauneau A, Lapierre C, Pollet B, Verhaegen D, Chaubet-Gigot N, et al: EgMYB2, a new transcriptional activator from Eucalyptus xylem, regulates secondary cell wall formation and lignin biosynthesis. Plant J. 2005, 43 (4): 553-567. 10.1111/j.1365-313X.2005.02480.x.View ArticlePubMedGoogle Scholar
- Patzlaff A, McInnis S, Courtenay A, Surman C, Newman LJ, Smith C, Bevan MW, Mansfield S, Whetten RW, Sederoff RR, et al: Characterisation of a pine MYB that regulates lignification. Plant J. 2003, 36 (6): 743-754. 10.1046/j.1365-313X.2003.01916.x.View ArticlePubMedGoogle Scholar
- Patzlaff A, Newman LJ, Dubos C, Whetten R, Smith C, McInnis S, Bevan MW, Sederoff RR, Campbell MM: Characterisation of PtMYB1, an R2R3-MYB from pine xylem. Plant Mol Biol. 2003, 53 (4): 597-608.View ArticlePubMedGoogle Scholar
- Legay S, Sivadon P, Blervacq AS, Pavy N, Baghdady A, Tremblay L, Levasseur C, Ladouce N, Lapierre C, Seguin A, et al: EgMYB1, an R2R3 MYB transcription factor from eucalyptus negatively regulates secondary cell wall formation in Arabidopsis and poplar. New Phytol. 2010, 188 (3): 774-786. 10.1111/j.1469-8137.2010.03432.x.View ArticlePubMedGoogle Scholar
- Taylor NG: Identification of cellulose synthase AtCesA7 (IRX3) in vivo phosphorylation sites–a potential role in regulating protein degradation. Plant Mol Biol. 2007, 64 (1–2): 161-171.View ArticlePubMedGoogle Scholar
- Chen S, Ehrhardt DW, Somerville CR: Mutations of cellulose synthase (CESA1) phosphorylation sites modulate anisotropic cell expansion and bidirectional mobility of cellulose synthase. Proc Natl Acd Sci USA. 2010, 107 (46): 17188-17193.View ArticleGoogle Scholar
- Morrison TA, Kessler JR, Hatfield RD, Buxton DR: Activity of two lignin biosynthesis enzymes during development of a maize internode. J Sci Food Agric. 1994, 65 (2): 133-139. 10.1002/jsfa.2740650202.View ArticleGoogle Scholar
- Bosch M, Mayer C-D, Cookson A, Donnison IS: Identification of genes involved in cell wall biogenesis in grasses by differential gene expression profiling of elongating and non-elongating maize internodes. Journal of experimental botany. 2011, 62 (10): 3545-3561. 10.1093/jxb/err045.PubMed CentralView ArticlePubMedGoogle Scholar
- Updegraff DM: Semimicro determination of cellulose inbiological materials. Analytical biochemistry. 1969, 32 (3): 420-424. 10.1016/S0003-2697(69)80009-6.View ArticlePubMedGoogle Scholar
- Hatfield RD, Wilson JR, Mertens DR: Composition of cell walls isolated from cell types of grain sorghum stems. J Sci Food Agric. 1999, 79 (6): 891-899. 10.1002/(SICI)1097-0010(19990501)79:6<891::AID-JSFA304>3.0.CO;2-#.View ArticleGoogle Scholar
- Gibeaut DM, Pauly M, Bacic A, Fincher GB: Changes in cell wall polysaccharides in developing barley (Hordeum vulgare) coleoptiles. Planta. 2005, 221 (5): 729-10.1007/s00425-005-1481-0.View ArticlePubMedGoogle Scholar
- Pettolino FA, Walsh C, Fincher GB, Bacic A: Determining the polysaccharide composition of plant cell walls. Nat Protoc. 2012, 7 (9): 1590-1607. 10.1038/nprot.2012.081.View ArticlePubMedGoogle Scholar
- Sims IM, Bacic A: Extracellular polysaccharides from suspension cultures of Nicotiana plumbaginifolia. Phytochemistry. 1995, 38 (6): 1397-1405. 10.1016/0031-9422(94)00832-E.View ArticleGoogle Scholar
- Dhugga KS, Barreiro R, Whitten B, Stecca K, Hazebroek J, Randhawa GS, Dolan M, Kinney AJ, Tomes D, Nichols S, et al: Guar seed beta-mannan synthase is a member of the cellulose synthase super gene family. Science. 2004, 303 (5656): 363-366. 10.1126/science.1090908.View ArticlePubMedGoogle Scholar
- Liepman AH, Nairn CJ, Willats WGT, Sorensen I, Roberts AW, Keegstra K: Functional genomic analysis supports conservation of function among cellulose synthase-like a gene family members and suggests diverse roles of mannans in plants. Plant Physiol. 2007, 143 (4): 1881-1893. 10.1104/pp.106.093989.PubMed CentralView ArticlePubMedGoogle Scholar
- Cantarel BL, Coutinho PM, Rancurel C, Bernard T, Lombard V, Henrissat B: The Carbohydrate-Active EnZymes database (CAZy): an expert resource for Glycogenomics. Nucleic Acids Res. 2009, 37 (Database issue): D233-238.PubMed CentralView ArticlePubMedGoogle Scholar
- Brown DM, Goubet F, Vicky WWA, Goodacre R, Stephens E, Dupree P, Turner SR: Comparison of five xylan synthesis mutants reveals new insight into the mechanisms of xylan synthesis. Plant J. 2007, 52 (6): 1154-1168. 10.1111/j.1365-313X.2007.03307.x.View ArticlePubMedGoogle Scholar
- Brown DM, Zhang Z, Stephens E, Dupree P, Turner SR: Characterization of IRX10 and IRX10‒like reveals an essential role in glucuronoxylan biosynthesis in Arabidopsis. Plant J. 2009, 57 (4): 732-746. 10.1111/j.1365-313X.2008.03729.x.View ArticlePubMedGoogle Scholar
- Mitchell RAC, Dupree P, Shewry PR: A novel bioinformatics approach identifies candidate genes for the synthesis and feruloylation of arabinoxylan. Plant Physiol. 2007, 144 (1): 43-53. 10.1104/pp.106.094995.PubMed CentralView ArticlePubMedGoogle Scholar
- Oikawa A, Joshi HJ, Rennie EA, Ebert B, Manisseri C, Heazlewood JL, Scheller HV: An integrative approach to the identification of Arabidopsis and rice genes involved in xylan and secondary wall development. PLoS One. 2010, 5 (11): e15481-10.1371/journal.pone.0015481.PubMed CentralView ArticlePubMedGoogle Scholar
- Pena MJ, Zhong RQ, Zhou GK, Richardson EA, O’Neill MA, Darvill AG, York WS, Ye ZH: Arabidopsis irregular xylem8 and irregular xylem9: Implications for the complexity of glucuronoxylan biosynthesis. Plant Cell. 2007, 19 (2): 549-563. 10.1105/tpc.106.049320.PubMed CentralView ArticlePubMedGoogle Scholar
- Persson S, Caffall KH, Freshour G, Hilley MT, Bauer S, Poindexter P, Hahn MG, Mohnen D, Somerville C: The Arabidopsis irregular xylem8 mutant is deficient in glucuronoxylan and homogalacturonan, which are essential for secondary cell wall integrity. Plant Cell. 2007, 19 (1): 237-255. 10.1105/tpc.106.047720.PubMed CentralView ArticlePubMedGoogle Scholar
- Cosgrove DJ: Expansive growth of plant cell walls. Plant Physiol Biochem. 2000, 38 (1–2): 109-124.View ArticlePubMedGoogle Scholar
- McQueen-Mason SJ, Cosgrove DJ: Expansin mode of action on cell walls (analysis of wall hydrolysis, stress relaxation, and binding). Plant Physiol. 1995, 107 (1): 87-100.PubMed CentralPubMedGoogle Scholar
- Zhang Q, Pettolino F, Dhugga KS, Rafalski A, Tingey S, Taylor J, Shirley N, Hayes K, Beatty M, Abrams SR, et al: Cell wall modifications in maize pulvini in response to gravitational stress. Plant Physiol. 2011, 156 (4): 2155-2171. 10.1104/pp.111.179606.PubMed CentralView ArticlePubMedGoogle Scholar
- Catala C, Rose JK, Bennett AB: Auxin regulation and spatial localization of an endo-1,4-beta-D-glucanase and a xyloglucan endotransglycosylase in expanding tomato hypocotyls. Plant J. 1997, 12 (2): 417-426. 10.1046/j.1365-313X.1997.12020417.x.View ArticlePubMedGoogle Scholar
- Fry SC, Mohler KE, Nesselrode B, Frankova L: Mixed-linkage beta-glucan: xyloglucan endotransglucosylase, a novel wall-remodelling enzyme from Equisetum (horsetails) and charophytic algae. Plant J. 2008, 55 (2): 240-252. 10.1111/j.1365-313X.2008.03504.x.View ArticlePubMedGoogle Scholar
- Hrmova M, Farkas V, Harvey AJ, Lahnstein J, Wischmann B, Kaewthai N, Ezcurra I, Teeri TT, Fincher GB: Substrate specificity and catalytic mechanism of a xyloglucan xyloglucosyl transferase HvXET6 from barley (Hordeum vulgare L.). The FEBS journal. 2009, 276 (2): 437-456. 10.1111/j.1742-4658.2008.06791.x.View ArticlePubMedGoogle Scholar
- Hrmova M, Farkas V, Lahnstein J, Fincher GB: A Barley xyloglucan xyloglucosyl transferase covalently links xyloglucan, cellulosic substrates, and (1,3;1,4)-beta-D-glucans. The Journal of biological chemistry. 2007, 282 (17): 12951-12962. 10.1074/jbc.M611487200.View ArticlePubMedGoogle Scholar
- Zhou H-L, He S-J, Cao Y-R, Chen T, Du B-X, Chu C-C, Zhang J-S, Chen S-Y: OsGLU1, a putative membrane-bound endo-1,4-b-D-glucanase from rice, affects plant internode elongation. Plant Mol Biol. 2006, 60 (1): 137-10.1007/s11103-005-2972-x.View ArticlePubMedGoogle Scholar
- Burton RA, Fincher GB: Current challenges in cell wall biology in the cereals and grasses. Frontiers in plant science. 2012, 3:Google Scholar
- Zhong R, Lee C, Ye Z-H: Evolutionary conservation of the transcriptional network regulating secondary cell wall biosynthesis. Trends Plant Sci. 2010, 15 (11): 625-632. 10.1016/j.tplants.2010.08.007.View ArticlePubMedGoogle Scholar
- Ye ZH, McCarthy RL, Zhong RQ: MYB83 Is a Direct Target of SND1 and Acts Redundantly with MYB46 in the Regulation of Secondary Cell Wall Biosynthesis in Arabidopsis. Plant Cell Physiol. 2009, 50 (11): 1950-1964. 10.1093/pcp/pcp139.View ArticlePubMedGoogle Scholar
- Ye ZH, McCarthy RL, Zhong RQ, Fowler S, Lyskowski D, Piyasena H, Carleton K, Spicer C: The poplar MYB transcription factors, PtrMYB3 and PtrMYB20, are involved in the regulation of secondary wall biosynthesis. Plant Cell Physiol. 2010, 51 (6): 1084-1090. 10.1093/pcp/pcq064.View ArticlePubMedGoogle Scholar
- Ye ZH, Zhong R, Richardson EA: The MYB46 transcription factor is a direct target of SND1 and regulates secondary wall biosynthesis in Arabidopsis. Plant Cell. 2007, 19 (9): 2776-2792. 10.1105/tpc.107.053678.PubMed CentralView ArticlePubMedGoogle Scholar
- Endler A, Persson S: Cellulose synthases and synthesis in arabidopsis. Mol Plant. 2011, 4 (2): 199-211. 10.1093/mp/ssq079.View ArticlePubMedGoogle Scholar
- Vanholme R, Demedts B, Morreel K, Ralph J, Boerjan W: Lignin biosynthesis and structure. Plant Physiol. 2010, 153 (3): 895-905. 10.1104/pp.110.155119.PubMed CentralView ArticlePubMedGoogle Scholar
- Faik A: Xylan biosynthesis: news from the grass. Plant physiology. 2010, 153 (2): 396-402. 10.1104/pp.110.154237.PubMed CentralView ArticlePubMedGoogle Scholar
- Pellny TK, Lovegrove A, Freeman J, Tosi P, Love CG, Knox JP, Shewry PR, Mitchell RA: Cell walls of developing wheat starchy endosperm: comparison of composition and RNA-Seq transcriptome. Plant physiology. 2012, 158 (2): 612-627. 10.1104/pp.111.189191.PubMed CentralView ArticlePubMedGoogle Scholar
- Mortimer JC, Miles GP, Brown DM, Zhang Z, Segura MP, Weimar T, Yu X, Seffen KA, Stephens E, Turner SR, et al: Absence of branches from xylan in Arabidopsis gux mutants reveals potential for simplification of lignocellulosic biomass. Proc Natl Acad Sci. 2010, 107 (40): 17409-17414. 10.1073/pnas.1005456107.PubMed CentralView ArticlePubMedGoogle Scholar
- Rennie EA, Hansen SF, Baidoo EE, Hadi MZ, Keasling JD, Scheller HV: Three members of the Arabidopsis glycosyltransferase family 8 are xylan glucuronosyltransferases. Plant physiology. 2012, 159 (4): 1408-1417. 10.1104/pp.112.200964.PubMed CentralView ArticlePubMedGoogle Scholar
- Anders N, Wilkinson MD, Lovegrove A, Freeman J, Tryfona T, Pellny TK, Weimar T, Mortimer JC, Stott K, Baker JM, et al: Glycosyl transferases in family 61 mediate arabinofuranosyl transfer onto xylan in grasses. Proc Natl Acad Sci. 2012, 109 (3): 989-993. 10.1073/pnas.1115858109.PubMed CentralView ArticlePubMedGoogle Scholar
- Chiniquy D, Sharma V, Schultink A, Baidoo EE, Rautengarten C, Cheng K, Carroll A, Ulvskov P, Harholt J, Keasling JD, et al: XAX1 from glycosyltransferase family 61 mediates xylosyltransfer to rice xylan. Proc Natl Acad Sci. 2012, 109 (42): 17117-17122. 10.1073/pnas.1202079109.PubMed CentralView ArticlePubMedGoogle Scholar
- Wilson SM, Burton RA, Doblin MS, Stone BA, Newbigin EJ, Fincher GB, Bacic A: Temporal and spatial appearance of wall polysaccharides during cellularization of barley (Hordeum vulgare) endosperm. Planta. 2006, 224 (3): 655-667. 10.1007/s00425-006-0244-x.View ArticlePubMedGoogle Scholar
- Rose JK, Braam J, Fry SC, Nishitani K: The XTH family of enzymes involved in xyloglucan endotransglucosylation and endohydrolysis: current perspectives and a new unifying nomenclature. Plant Cell Physiol. 2002, 43 (12): 1421-1435. 10.1093/pcp/pcf171.View ArticlePubMedGoogle Scholar
- Mohler KE, Simmons TJ, Fry SC: Mixed‒linkage glucan: xyloglucan endotransglucosylase (MXE) re‒models hemicelluloses in Equisetum shoots but not in barley shoots or Equisetum callus. New Phytol. 2013, 197 (1): 111-122. 10.1111/j.1469-8137.2012.04371.x.View ArticlePubMedGoogle Scholar
- Schober MS, Burton RA, Shirley NJ, Jacobs AK, Fincher GB: Analysis of the (1, 3)-β-D-glucan synthase gene family of barley. Phytochemistry. 2009, 70 (6): 713-720. 10.1016/j.phytochem.2009.04.002.View ArticlePubMedGoogle Scholar
- McWilliams DA, Berglund DR, Endres GJ: Corn growth and managementquick guide. In vol. A-1173. North Dakota: North Dakota State University; 1999.Google Scholar
- Ciucanu I, Kerek F: A simple and rapid method for the permethylation of carbohydrates. Carbohy Res. 1984, 131 (2): 209-217. 10.1016/0008-6215(84)85242-8.View ArticleGoogle Scholar
- Filisetti-Cozzi TMCC, Carpita NC: Measurement of uronic acids without interference from neutral sugars. Analytical biochemistry. 1991, 197 (1): 157-162. 10.1016/0003-2697(91)90372-Z.View ArticlePubMedGoogle Scholar
- Hayes KR, Beatty M, Meng X, Simmons CR, Habben JE, Danilevskaya ON: Maize global transcriptomics reveals pervasive leaf diurnal rhythms but rhythms in developing ears are largely limited to the core oscillator. PloS one. 2010, 5 (9): e12887-10.1371/journal.pone.0012887.PubMed CentralView ArticlePubMedGoogle Scholar
- Burton RA, Shirley NJ, King BJ, Harvey AJ, Fincher GB: The CesA gene family of barley, quantitative analysis of transcripts reveals two groups of Co-expressed genes. Plant Physiol. 2004, 134 (1): 224-236. 10.1104/pp.103.032904.PubMed CentralView ArticlePubMedGoogle Scholar
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