Reprogramming of gene expression during compression wood formation in pine: Coordinated modulation of S-adenosylmethionine, lignin and lignan related genes
© Villalobos et al. 2012
Received: 12 January 2012
Accepted: 29 June 2012
Published: 29 June 2012
Transcript profiling of differentiating secondary xylem has allowed us to draw a general picture of the genes involved in wood formation. However, our knowledge is still limited about the regulatory mechanisms that coordinate and modulate the different pathways providing substrates during xylogenesis. The development of compression wood in conifers constitutes an exceptional model for these studies. Although differential expression of a few genes in differentiating compression wood compared to normal or opposite wood has been reported, the broad range of features that distinguish this reaction wood suggest that the expression of a larger set of genes would be modified.
By combining the construction of different cDNA libraries with microarray analyses we have identified a total of 496 genes in maritime pine (Pinus pinaster, Ait.) that change in expression during differentiation of compression wood (331 up-regulated and 165 down-regulated compared to opposite wood). Samples from different provenances collected in different years and geographic locations were integrated into the analyses to mitigate the effects of multiple sources of variability. This strategy allowed us to define a group of genes that are consistently associated with compression wood formation. Correlating with the deposition of a thicker secondary cell wall that characterizes compression wood development, the expression of a number of genes involved in synthesis of cellulose, hemicellulose, lignin and lignans was up-regulated. Further analysis of a set of these genes involved in S-adenosylmethionine metabolism, ammonium recycling, and lignin and lignans biosynthesis showed changes in expression levels in parallel to the levels of lignin accumulation in cells undergoing xylogenesis in vivo and in vitro.
The comparative transcriptomic analysis reported here have revealed a broad spectrum of coordinated transcriptional modulation of genes involved in biosynthesis of different cell wall polymers associated with within-tree variations in pine wood structure and composition. In particular, we demonstrate the coordinated modulation at transcriptional level of a gene set involved in S-adenosylmethionine synthesis and ammonium assimilation with increased demand for coniferyl alcohol for lignin and lignan synthesis, enabling a better understanding of the metabolic requirements in cells undergoing lignification.
Large amounts of wood can be formed throughout the life of a tree through a complex process of cell differentiation called xylogenesis. In this process, cambium-derived cells undergo cell division followed by thickening of the secondary cell wall by modification of the synthesis and deposition of cellulose, hemicelluloses, cell wall proteins and lignin, and finally programmed cell death to develop tracheary elements . Genes involved in these cellular processes are under strict transcriptional regulation during different stages of differentiation . Nevertheless, inputs from external cues are also integrated in this developmental program to adapt secondary xylem properties to growth requirements in a continuously changing environment . As a result of this interaction, natural variations are found in wood properties not only among different species and genotypes, but also within the same tree .
Transcriptome analysis of differentiating secondary xylem has allowed us to draw a general picture of the genes, metabolic pathways and potential regulators involved in wood formation [5–11]. However, our knowledge is limited as to how the transcriptomes, proteomes and metabolomes involved in wood development are modulated by developmental and environmental signals to cause within-tree variation in wood properties. Considerable effort has been focused on studying the main pathways that lead to monolignol biosynthesis  and carbohydrate partitioning to cellulose , as well as understanding how changes in gene expression in those pathways may affect cellular wall characteristics and, consequently, wood quality . However, less attention has been paid to the pathways that provide S-adenosylmethionine (SAM) for methylation reactions during biosynthesis of coniferyl and sinapyl alcohols, even though transcripts and proteins for enzymes of these pathways are abundant in the developing xylem [15, 16]. Consumption of methyl units during lignification also implies the existence of an important carbon sink, and modifications in the availability of SAM may affect wood quality through alterations in lignin content and composition [16–18]. Furthermore, it has been proposed that glycine decarboxylase activity associated with SAM metabolism could be an important source of released ammonium, which must be efficiently re-assimilated to prevent significant imbalances in the strict nitrogen economy of the plant .
Molecular determinants of intra-genotype variation can be identified by comparing transcriptomes from cambial derivatives undergoing differentiation in the same tree that produce wood that differs in composition and structure . However, the plasticity of the molecular machinery involved in wood formation  may result in some difficulties in terms of defining candidate genes when expression patterns are compared over different annual growth periods. Therefore, the definition of a consistent set of candidate genes for wood property variations requires analysis that mitigates sources of variation from genotypes and local environmental changes.
Reaction wood illustrates how the integration of environmental signals into the secondary xylem developmental program leads to intra-genotype variation in wood. When the stem of a woody plant grows in a non-vertical orientation it forms reaction wood, a specialized secondary xylem that helps the stem maintain a certain orientation and re-orients growth . In gymnosperms, reaction wood is called compression wood and it develops on the underside of branches and inclined stems . Cell walls in compression wood tracheids are thicker than in normal wood and lack the innermost S3 layer. It also contains more lignin, less cellulose and altered levels of hemicelluloses than normal wood. Moreover, in compression wood cellulose microfibrils are deposited with increased angle relative to the cell axis [22, 23], and the lignin is enriched in p-hydroxyphenylpropane units [24, 25]. In contrast, opposite wood develops on the opposite side of the inclined stem and it is more similar to normal wood . Differential expression of a few genes during compression wood differentiation compared to normal or opposite wood has been reported [16, 26–28]. However, the clear anatomical, structural and compositional differences that characterize compression wood suggest that the expression of more genes would be modified during its differentiation [25, 29, 30].
We are interested in how biosynthetic pathways that provide substrates for xylogenesis are coordinated and regulated according to the different demands during development of wood with distinct composition. In particular, comparison of samples from differentiating compression wood and opposite wood from the same tree allows us to analyze the transcriptome changes accompanying to different levels of lignin deposition during xylogenesis. In this work, we present the results of a comparative transcriptomic analysis that comprehensively uses a range of cDNA libraries and microarray analyses, combining samples from different Pinus pinaster provenances collected in different years and geographic locations, to identify changes in the transcriptome associated with compression wood development.
Identification of genes differentially expressed during compression and opposite wood formation in Pinus pinaster
Sequences with an average Phred score >20 per nucleotide in a sliding window of 15 nucleotides and a minimal length of 100 nucleotides were kept for further analysis (average length of 437 nucleotides and a standard deviation of ±171). Those with lower quality scores or shorter than 100 nucleotides were re-sequenced. The complete set of sequences corresponding to differentially expressed genes from microarray 1 and 2 were used to define a set of unigenes, and a total number of 355 unigenes up-regulated in Cx and 176 unigenes up-regulated in Ox were obtained. Moderate values of sequence redundancy were obtained (31.6% for Cx and 21.2% for Ox).
Trancriptome changes in functional categories related to cell wall during compression wood formation in pine
The complete set of unigenes was functionally annotated using BlastX analysis  against GenBank and BlastN using the Pine Gene Index database (Additional file 3). Sequences that matched with the same entry in the database were assumed to represent the same gene. Therefore, the final numbers of unigenes were reduced to 331 for Cx and 165 for Ox. Most of these genes showed significant similarities to sequences in databases (293 in Cx and 145 in Ox), although some of them were similar to sequences with unknown function (49 in Cx and 45 in Ox). The number of unigenes with no significant similarity was low in both cases (38 in Cx and 20 in Ox).
The functional categories with larger numbers of up-regulated genes in Cx compared to Ox are consistent with structural and chemical modifications of the cell wall, and as shown in Additional file 3 (“Up-regulated in Cx” tab) include genes encoding cellulose synthase subunits (contigs 19 and 7S, singletons BX249614 and FN256963), sucrose synthase (contigs 12 and 35S), cellulose synthase-like A (contig 19S), glycosyltransferases (contig 4P, singleton BX250177), xyloglucan galactosyltransferase (singleton FN256497), α- and β-tubulins (contigs 13, 7P, 31S and 51S, singletons BX255503, FN256632, FN256674, FN256784, BX255285, BX249611 and FN256695) and a putative microtubule-associated protein (singleton BX253390). In particular, the gene encoding xyloglucan galactosyltransferase (XGT) showed a high level of expression in Cx, whereas transcripts were undetectable in Ox (Figure 4b, XGT).
Transcripts for enzymes involved in lignin biosynthesis were also up-regulated in Cx (Additional file 3, “Up-regulated in Cx” tab), including those encoding enzymes in the monolignol biosynthetic pathway, such as phenylalanine ammonia lyase (PAL: contig 3S, singletons BX249569, BX253670 and FN257113), p-coumarate 3-hydroxylase (C3H: singleton BX248886), 4-coumarate:CoA ligase (4CL: singletons BX255483 and BX253310), cinnamyl alcohol dehydrogenase (CAD: contig 2P, singleton BX253572), hydroxycinnamoyl-CoA:shikimate hydroxycinnamoyl transferase (HCT, singleton FN256636), caffeoyl-CoA-O-methyltransferase (CCoAOMT, singleton FN256577) and caffeate O-methyltransferase (COMT, contig 19P).
Several genes up-regulated in Cx and classified in the functional category “amino acid metabolism” encode enzymes involved in the synthesis of precursors for monolignol biosynthesis, such as the enzymes of the main trunk of the shikimate pathway chorismate synthase (contig 5, singleton FN256628), 3-dehydroquinate dehydratase/shikimate 5-dehydrogenase (contig 22), shikimate kinase (singleton BX251461) and 5-enolpyruvylshikimate 3-phosphate synthase (singleton BX252482). In particular, the expression pattern was confirmed by northern blot for the genes encoding chorismate synthase, and 3-dehydroquinate dehydratase/shikimate 5-dehydrogenase (Figure 4a, CS and DHQ/SDH, respectively).
Expression of genes encoding enzymes related to SAM biosynthesis in cells undergoing xylogenesis
Genes related to S-adenosylmethionine (SAM) metabolism were also widely represented among those up-regulated in Cx and classified in the functional category “amino acid metabolism” (Additional file 3, “Up-regulated in Cx” tab). SAM is a universal methyl donor for many different cellular metabolic reactions, including those catalyzed by CCoAOMT and COMT. Both enzymes are essential for the biosynthesis of coniferyl and sinapyl alcohols, precursors of lignin, lignans and other phenylpropanoids . Therefore, the higher lignin content of compression wood may require a larger supply of SAM during development compared to opposite wood.
Expression of genes encoding enzymes related to lignan-biosynthesis in cells undergoing xylogenesis
Comparative transcriptome analysis shows reprogramming of cell wall related genes during compression wood formation in pine
In this work, we carried out a comparative transcriptome analysis between developing compression and opposite wood using a combination of differently constructed cDNA libraries and microarray analyses (Figure 1). Samples from three unrelated provenances, different geographic location or collected in different years (Figure 2) were integrated in the analysis to mitigate the potential effects of variability triggered by genotypic or environmental differences in order to identify a consistent set of candidate genes for wood properties.
The external stimulus that leads to the formation of compression wood caused significant changes of gene expression, as revealed by the large number of genes that were up-regulated or down-regulated in Cx compared to Ox (Figure 3) and the specific expression of some genes in Cx (Figure 4). An important component of this gene reprogramming is clearly related to the chemical and structural modifications of the thick secondary cell wall characteristic of conifer reaction wood, as suggested by the over-represented functional categories among the up-regulated genes in Cx, such as biogenesis of cytoskeleton, biogenesis of cell wall components, secondary metabolism, cellular transport and C-compound and carbohydrate metabolism (Figure 5 and Additional file 3).
A parallel up-regulation of genes encoding cellulose synthase subunits and sucrose synthase in Cx compared to Ox was observed, suggesting a higher rate of cellulose biosynthesis during compression wood formation. It has been well documented that the relative content of cellulose in compression wood is lower than in normal wood and opposite wood [21, 38]. However, the S2 layer of secondary cell walls in compression wood is thicker than in normal and opposite wood, which contributes to the final thickness of the tracheid cell wall . Therefore, in terms of absolute quantity, the development of compression tracheids may require higher rates of cellulose synthesis.
Different genes encoding α- and β-tubulins were also up-regulated during compression wood formation. Up-regulation of α-tubulin during compression wood formation in Pinus taeda has been reported previously , which supports our findings. Different lines of experimental evidence suggest that cortical microtubules of the cytoskeleton are involved in secondary cell wall pattern deposition and cellulose microfibril orientation [39, 40]. We also identified a gene up-regulated in Cx that encodes a putative microtubule-associated protein (MAP). Several MAPs have been investigated  and their involvement in regulating cellulose microfibril angle (MFA) has been revealed in Arabidopsis MAP mutants, which show altered MFA in fiber walls [42, 43]. More recently, it has been demonstrated that microtubule-associated protein AtMAP70-5 regulates secondary cell wall patterning in Arabidopsis. Differential expression of these genes may contribute to the remarkable variation of MFA in the S2 cell wall layer between compression and opposite or normal wood, which plays a key role in the different mechanical properties of both types of wood [20, 21, 29, 45].
Another group of genes that are up-regulated during compression wood differentiation encode enzymes that could be involved in the biosynthesis of hemicellulose, including a cellulose synthase-like, two glycosyltransferases and a xyloglucan galactosyltransferase. Although xyloglucan is a hemicellulose characteristic of primary cell walls, it has been suggested that modifications in xyloglucan may be related to the reinforcement of connections between primary and secondary wall layers . In particular, the gene encoding a putative xyloglucan galactosyltransferase seems to be specifically induced during Cx formation (Figure 4bXGT and data not shown). In contrast, two genes encoding a putative xyloglucan endotransglucosylase/hydrolase are downregulated in Cx compared to Ox (Additional file 3, “Up-regulated in Ox” tab and Figure 4xbXET). Therefore, our comparative transcriptome analysis suggests specific modifications of hemicellulose biosynthesis during compression wood development.
Consistent with the enrichment of lignin in compression wood , we found that genes encoding enzymes of the monolignol biosynthetic pathway were up-regulated in Cx (Additional file 3, “Up-regulated in Cx” tab), such as phenylalanine ammonia-lyase (PAL), 4-coumarate:CoA ligase (4CL), p-coumarate-3-hydroxylase (C3H), cinnamyl-alcohol dehydrogenase (CAD) hydroxycinnamoyl-CoA:shikimate hydroxycinnamoyl transferase (HCT), caffeoyl-CoA-O-methyltransferase (CCoAOMT) and caffeate O-methyltransferase (COMT). In addition, the biosynthesis of monolignols demands substrates such as phenylalanine, shikimate and S-adenosylmethionine (SAM), which are provided by different metabolic reactions . The quantitative importance of the shikimate and SAM metabolic pathways in the context of a highly lignified tissue, such as compression xylem, is supported by the fact that 22 of the 26 genes up-regulated in Cx that were classified in the “amino acid metabolism” functional category encode enzymes in these pathways (Additional file 3, “Up-regulated in Cx” tab).
In agreement with the elevated levels of shikimate in compression wood compared to normal wood that has been reported  and the higher demand of this substrate for monolignol biosynthesis, our microarray analyses showed that four genes encoding enzymes in the main trunk of the shikimate pathway were up-regulated in Cx (chorismate synthase, 3-dehydroquinate dehydratase/shikimate 5-dehydrogenase, shikimate kinase and 5-enolpyruvylshikimate 3-phosphate synthase).
Transcriptional adaptation of SAM biosynthetic pathway to the metabolic demand of coniferyl alcohol during xylogenesis
SAM is a methyl-group donor for coniferyl alcohol biosynthesis in conifers, and for both coniferyl and sinapyl alcohol in angiosperms . Genes involved in lignin biosynthesis and those encoding enzymes of the activated methyl cycle were shown to be more highly expressed in the woody core tissue of hemp . According to this functional relationship, genes encoding the enzymes of the activated methyl cycle (MS, SAMS and SAHH) were also up-regulated in Cx (Additional file 3 and Figure 6). Moreover, six additional genes were also up-regulated in Cx that encode enzymes located in three different cellular compartments, which are involved in providing a continuous supply of methyl groups from serine into the cycle (Figure 6).
Two of these genes encode cytosolic serine hydroxymethyltransferase (cSHMT) and methylenetetrahydrofolate reductase (MTHFR), which catalyse the conversion of serine to glycine with the concomitant transfer of a methyl group to the tetrahydrofolate to produce 5,10 methylenetetrahydrofolate and the reduction of 5,10-methylenetetrahydrofolate (CH2-THF) to 5-methyltetrahydrofolate (CH3-THF) respectively (Figure 6). Genes encoding H-protein subunit of the mitochondrial glycine decarboxylase complex (GDCH) and the mitochondrial serine hydroxymethyltransferase (mSHMT) are also included in this functional group. The essential function of the mitochondrial glycine decarboxylase/serine hydroxyl methyltransferase complex in C1 metabolism has been previously described . Glycine catabolism and recycling to serine by GDC/SHMT complex prevents the accumulation of glycine under high rates of SAM synthesis. The accumulation of glycine would push the cSHMT reaction toward the formation of serine and inhibit SAM synthesis . H-protein is a critical element in the sequence of reactions in the GDC complex, acting as a mobile substrate for the other enzymatic components, and changes in the levels of H-protein may modulate the activity of the complex . Different genes encoding H-protein have been found in Populus, and transcripts encoding individual isoforms were specifically abundant in developing xylem, suggesting the association of distinct isoforms with photorespiration and C1 metabolism . Finally, genes encoding plastid enzymes 3-phosphoglycerate dehydrogenase (PGDH) and phosphoserine aminotransferase (PSAT) are involved in serine biosynthesis from 3-phophoglycerate , which would supply the high demand of this amino acid that is required for SAM synthesis during lignification.
The coordinated modulation of SAM and monolignol biosynthetic genes with lignin accumulation was also supported by two additional observations. First, the smallest differences in transcript abundances between Cx and Ox were observed for tree T4-08 (Figure 6), which also showed the smallest differences in lignin content (Figure 2b). Second, the relative transcript abundance of these genes during in vitro tracheid differentiation was parallel to lignin content (Figure 7). The increase in the levels of all enzymes involved in SAM synthesis may allow an increased flux through the pathway to supply the massive demand of methyl groups during lignification, with the minimal impact on metabolite levels . In conclusion, these data strongly suggest that up-regulation of SAM metabolism genes during compression wood formation is due to an increased demand for methyl groups in coniferyl alcohol biosynthesis. However, SAM also acts as the precursor in the biosynthesis of the polyamines spermidine and spermine, the metal ion chelating compounds nicotianamine and the plant hormone ethylene. When acting as a precursor of these molecules, SAM is recycled from released 5´-methylthioadenosine through the Yang cycle , but genes encoding enzymes of this pathway were not found among those up-regulated in Cx.
As a result of the activity of mitochondrial GDC during lignification the release of significant amounts of ammonium should be expected (Figure 6), in addition to the ammonium released in the reaction catalysed by PAL. The massive ammonium release could compromise nitrogen economy in a woody perennial during secondary growth if it is not efficiently recycled . It appears that in order to cope with the high amounts of ammonia released by PAL and GDC activities during lignification a glutamine synthetase gene (GS1b) was up-regulated in Cx and during in vitro tracheid differentiation (Figure 6 and Figure 7). This gene has been functionally associated with ammonia assimilation in vascular tissues of seedlings [35, 54].
In conifers, lignin lacks sinapyl alcohol, and coniferyl alcohol is the most abundant monolignol  in the polymer. Compression wood is relatively enriched in H subunits, and an increase in p-glucocoumaryl alcohol is associated with development of this reaction wood . Nevertheless, the increased level of transcripts for enzymes involved in SAM synthesis in Cx indicates a higher demand for coniferyl alcohol to respond to an overall increase in lignin production, which is consistent with the reported higher abundance of coniferin residues in compression wood relative to normal wood in Pinus taeda. However, an additional fate for coniferyl alcohol is the synthesis of lignans . Three genes encoding enzymes involved in coniferyl alcohol-derived lignan metabolism were also up-regulated in Cx compared with Ox and in cells that were induced to differentiate into tracheids in vitro compared to non-induced cells (Additional file 3, Figure 8): pinoresinol-lariciresinol reductase (PLR), phenylcoumaran benzylic ether reductase (PCBER) and phenylpropenal double-bond reductase (PPDBR). These results suggest that during compression wood formation an increased demand for coniferyl alcohol residues may also be related to an increase in the biosynthesis of lignans. Lignans have been related to defense and heartwood formation . Moreover, PCBER is a prominent poplar xylem protein that is strongly associated with lignifying cells , and a general function for PCBER has been proposed in lignifying tissues and wood development. Lignans may be infused in the secondary cell wall during lignification to cope with the oxidative stress accompanying lignin polymerization , which may explain the enhanced expression of lignan biosynthesis genes during compression wood formation and in vitro tracheid differentiation.
Our strategy for comparative transcriptomic analysis in pine Cx and Ox has revealed a broad spectrum of changes in the transcriptome of differentiating xylem cells, consistent with the formation of wood with different structures and compositions. This work provides a resource for further characterization of molecular components that determine variation in softwood properties. In particular, the coordinated modulation of expression that was observed for genes involved in serine, SAM, monolignol and lignan biosynthesis, and the central role of glutamine synthetase to avoid N deficiency are important for understanding plant metabolic requirements and regulation during intensive lignification, and should thus be considered in strategies for lignin bioengineering.
To construct the different cDNA libraries for microarray manufacturing, P. pinaster samples of compression (Cx), opposite (Ox), early (Ex) and late (Lx) developing xylem were collected from different genotypes of a Corsican clonal population planted in 1986 in the forestry station of INRA-Pierroton (Aquitaine, France). Compression wood was induced by bending the stem at an angle of 15° away from the vertical, and 12 samples were collected at the beginning (early wood) and at the end (late wood) of the growing season in 1998 and 1999 (after 8 days, 40 days, 120 days and 1.5 year of starting the stimulus) and 2000 (after 6 hours and 1 days after starting the stimulus). Cx was sampled from the underside of the bent trunk and Ox from the upper side. Ex and Lx samples were collected from a 14-year-old straight tree in April and August 1999, respectively. Juvenile (Jx) and Mature (Mx) developing xylem were sampled in 2001 from the crown and the base (breast height) of the stem in a 30-year-old maritime pine tree from the Aquitaine provenance.
For microarray and northern hybridizations, samples of Cx and Ox were collected from four maritime pine trees between 25 and 35 years old (T1-05, T2-05, T3-05 and T4-05) in May 2005 in Sierra Bermeja (Estepona, Spain). For real-time quantitative PCR analyses (qRT-PCR), samples of Cx and Ox were collected in May 2008 in Sierra Bermeja from four different trees (T1-08, T2-08, T3-08 and T4-08). Cx was induced by bending the tree stem at an angle of 45° for 60 days before sampling. Developing xylem was scraped with a scalpel after removing bark and phloem. Samples were immediately frozen in liquid nitrogen after harvesting and stored at -80 °C until use.
Development of Pinus pinaster calli and in vitro differentiation of tracheids
Calli were developed from Pinus pinaster hypocotyl explants using the procedures and culture media described by Möller et al.. To induce tracheids, callus cells were suspended in EDM liquid medium and transferred to induction media following the same procedure as described by Möller et al., except that the induction medium was EDM medium without hormones instead of EDM medium supplemented with activated charcoal. EDM medium with hormones was inoculated in parallel as a control medium.
Tissue preparation and phloroglucinol staining for light microscopy
Xylem scrapings were fixed by the freeze substitution method . Tissue pieces were embedded in Paraplast (Leica Microsystems) at 42 °C in a progression series with Histo-Clear and then incubated six times in Paraplast at 62 °C for 8 h. Sections (10 μm) were then obtained from embedded tissues with a Leitz microtome (Ernst Leitz, Midland, Ontario, Canada) and directly mounted onto poly-L-Lys-coated glass slides. Sections were stained with phloroglucinol (Sigma-Aldrich) following the procedure described elsewhere  and visualized under light microscopy, using a Nikon Eclipse E 800 microscope.
Cell wall preparation and lignin quantification was performed following the method described by Lange et al.. For cell wall preparation 100 mg of tissue was used.
Isolation of RNA
Total RNA was isolated following the method of Chang et al.. RNA concentration and purity was determined by spectrophotometry and integrity was confirmed by electrophoresis on denaturing agarose/formaldehyde gels.
Construction of cDNA libraries
The cDNA probes for microarray construction were obtained from two different sources. A composite cDNA library was constructed from a mixed pool of equal amounts of total RNA extracted from samples of the Corsican provenance described above, including Ex, Lx and the Cx and Ox samples from artificially bent trees for different periods of time (from 6 hours to 1.5 years). PolyA(+) RNA was isolated from the mixed pool of total RNA, and the cDNA library was constructed using the λ-ZAP-cDNA synthesis kit (Stratagene, La Jolla, CA, USA).
The second source of cDNA probes was four subtractive cDNA libraries constructed from samples of the Corsican provenance by the suppression subtractive hybridization method (SSH), using the PCR-Select cDNA Subtraction Kit (Clontech, Palo Alto, CA, USA). Two SSH libraries were produced using cDNAs from Cx and Ox by performing the subtraction procedure in both directions. The same procedure was followed to obtain two SSH libraries with samples of Jx and Mx. Subtracted cDNAs were cloned in pGEM®-T Easy plasmid (Promega, Madison, WI, USA), transformed into Escherichia coli JM109 (Promega) or XL1Blue (Stratagene, La Jolla, CA, USA) and plated on LB plates containing 100 μg/mL ampicillin, 1 mM IPTG and 80 μg/mL X-gal. White colonies were selected from each library and separately cultured in 96-well plates containing LB with ampicillin.
Construction of cDNA microarrays
To construct cDNA microarray 1, 2800 inserts from the composite λ-ZAP cDNA library were PCR-amplified using T3 and T7 primers or M13 Forward and M13 Reverse primers. PCR products were purified with 96-well multiscreen filter plates (Millipore Corp. Bedford, MA, USA). Amplified cDNAs were checked on agarose gel electrophoresis after purification. Solutions of purified-cDNA probes in 50% DMSO were prepared to a concentration between 100 and 200 ng/μl, and stored at -20 °C until use. Each cDNA probe was printed in duplicate onto ULTRA gaps II coated slides (Corning Inc., NY, USA) using a Qarray2 (Genetix Ltd, Queensway, UK) with a telechem printing head and 16 split pins (Biorobotics, Cambridge, UK), and with a 4 x 4 configuration. As a control, ArrayControl Sense Oligo Spots (spikes) (Ambion Inc., Austin, TX, USA) were included. After printing, the slides were dried at room temperature and the spotted cDNA were cross-linked to the slide surface by UV irradiation at 300 mJ/cm2.
For cDNA microarray 2, 4041 cDNA clones from the four SSH libraries described above were randomly selected and cDNAs inserts were amplified by PCR using Nested PCR primers 1 and 2R included in the PCR-select cDNA subtraction kit (Clontech, Palo Alto, CA, USA). PCR-amplified cDNA were purified and spotted in duplicate as described above.
Microarray hybridization, scanning and data acquisition
Dye labeled aRNA was synthesized with the Amino allyl MessageAmp II aRNA amplification kit (Ambion Inc., Austin, TX, USA). Prehybridization, hybridization, and posthybridization washes were carried out using Pronto!™ Universal Hybridization Kit (Corning Inc.) in a HS 400 Pro hybridization station (Tecan Trading AG, Switzerland). Five micrograms of each of the labeled aRNA targets was added to the hybridization solution and denatured at 95 °C for 5 min. The slides were hybridized for 16 h at 42 °C. Hybridized slides were scanned with 5 μm resolution, and signal intensities were detected with a Q-Scan scanner (Genetix).
Microarray data analysis
Four dual-target hybridizations were performed using labeled aRNA targets from Cx and Ox samples from different individual pine trees (T1-05, T2-05, T3-05 and T4-05), including two dye-swap experiments. Since every slide was printed with two full replicates of the microarray, each microarray data set consisted of four dye-balanced hybridizations for each type of xylem in duplicate. Spots flagged below 0 using GenePix v6.0 software (Axon Instruments) and those with signal intensities that did not surpass 2X the background signal in both channels were discarded. Background correction was performed with the “normexp” method of the limma library. The M value was defined as the base two logarithm of every expression ratio, computed as the ratio between the background-corrected foreground intensities of the Cy3 and Cy5 channels. Raw expression data were normalized for all sources of systematic variation with the print-tip loess , using the common assumption of considering the whole microarray expression as invariant. Scaling between arrays was not needed. Gene significance was then estimated using a robust linear model corrected by a moderated t-test (empirical Bayes) . The multi-testing effect was corrected adjusting p-values by the Benjamini and Hochberg method . A gene was considered significantly up- or down-regulated if it met these two criteria: (1) adjusted p ≤ 0.001; and (2) fold change ≥ 1.5. The Biobase v 2.0.1 of the Bioconductor package  was installed under R version 2.7.1 for all statistical analysis, mainly the limma v 2.14.5  and marray v 1.18.0 libraries (http://www.bioconductor.org/packages/release/bioc/html/marray.html). The outputs of microarray analyses carried out in this study are available at Gene Expression Omnibus data repository (GEO accession numbers GSE37678 and GSE37736). All data are MIAME compliant.
Sequencing and sequence analysis
A total of 12,134 plasmid clones from the composite cDNA library were sequenced by single pass from the 5´-end with the T3 primer, which rendered 8429 ESTs. These sequences were pre-processed and assembled into unigenes before proceeding to functional annotation as described elsewhere . Sequencing of cDNA clones from the SSH libraries from genes that were differentially expressed in Cx and Ox according to microarray 2 data were carried out using M13 forward, SP6 or T7 primers. Vector and adapter sequences were deleted using SeqTrim . Sequences with an internal RsaI site were discarded and not considered for contig assembly, as they were supposed to contain fusions of two cDNA fragments. All the sequences were deposited in the EMBL Nucleotide Sequence Database (accession numbers are listed in Additional file 3).
Contigs were established using CAP3 . Non-redundant cDNA sequences after EST assembly were annotated by BLASTX at GenBank and classified into functional groups using data reported in the literature and MIPS functional catalogue . Only BLASTX hits with E-values ≤ 1x10-10 and a minimum of 50% similarity were selected for annotation. Sequences showing weak similarity (E-value > 1x10-10) and those without significant similarity were compared by BLASTN algorithm with the Pine Gene Index database (http://compbio.dfci.harvard.edu/tgi/cgi-bin/tgi/gimain.pl?gudb=pine). The resulting pine tentative contigs (TCs) or pine ESTs, which shared more than 90% of identity with each query sequence, were used as new queries for BLASTX at GenBank.
Northern blot analysis
Seven micrograms of total RNA from Cx or Ox were analyzed by Northern blot as previously described . 32P labeled probes of selected genes were produced with the High Prime System (Roche Diagnostics). Prehybridizations and hybridizations were performed at 65 °C. Hybridized membranes were washed with 1X SSC, 0.1% SDS and 0,1X SSC, 0.1% SDS at 65 °C.
Real-time quantitative PCR analysis (qRT-PCR)
RNA samples were treated with RNase-Free rDNase to eliminate genomic DNA contamination and then purified using NucleoSpin RNA clean-up (Macherey-Nagel, Dürem, Germany). The quality of the treated RNA was checked by both gel electrophoresis and spectrophotometry. Reverse transcription using 1 μg of total RNA was carried out with iScript cDNA Synthesis Kit (Bio-Rad Laboratories, CA, USA).
Sense and antisense primers were designed for the specific amplification of selected genes. The sequences of the primers are shown in Additional file 5. PCR reactions were performed in a Stratagene MxPro 3000P Real-Time PCR System (Stratagene). Reactions were performed in 25 μL containing Quantimix easy master mix (Quantimix Easy SYG kit, BioTools B&M Labs, S.A., Madrid, Spain), 0.4 μM of each primer and 10 ng of cDNA (RNA equivalent). PCRs were performed by incubation 2 min at 95 °C followed by 40 cycles of 30 s at 95 °C, 30 s at specific annealing temperature and 15 s at 72 °C. Fluorescence was measured at the end of each extension step. Three technical replicates were analyzed for each sample. The specificity of each amplification reaction was verified by melting point analysis at the end of each experiment, and during protocol development by gel electrophoresis. In every assay negative controls were included with RNA not reverse transcribed from the different analyzed samples or without template to rule out contaminations due to remaining genomic DNA or sample manipulations.
The values of amplification efficiency, Ct and initial fluorescence (R0) for every reaction were calculated with the Miner algorithm . Relative expression levels were obtained from the ratio between R0 of the target gene and a normalization factor. To determine the normalization factor, the relative transcript abundances of five genes with fold change value of 1 in the microarray analyses were also determined by qRT-PCR (see Additional file 5 for primer sequences) and analyzed with the geNorm algorithm  to select the combination of more stable genes in every experiment. For Cx versus Ox comparison the geometric mean of R0 obtained for ribosomal protein L34 and actin was used. For the analysis of relative transcript abundance during in vitro development of tracheids the geometric mean of R0 values for the genes encoding 40 S ribosomal protein S27, Ubi-like protein and elongation factor 1α was used.
We are grateful to Remedios Crespillo and Dr. Mónica Pérez Alegre for their technical assistance. We also thank Noé Fernández Pozo for the help with the submission of the sequences to the EMBL database, and Dr. Kaisa Nieminen for proofreading the manuscript. This work was supported by grants from Ministerio de Educación y Ciencia (AGL2006-07360 and AGL2009-12139-C02-02) Spain, and research funds from Junta de Andalucía (BIO-114). DPV was supported by a predoctoral fellowship from Junta de Andalucía (Spain), SMD-M and E-SSS were supported by pre-doctoral fellowships from Ministerio de Educación y Ciencia (Spain).
- Turner S, Gallois P, Brown D: Tracheary element differentiation. Annu Rev Plant Biol. 2007, 58: 407-433. 10.1146/annurev.arplant.57.032905.105236.PubMedView ArticleGoogle Scholar
- Schrader J, Nilsson J, Mellerowicz E, Berglund A, Nilsson P, Hertzberg M, Sandberg G: A high-resolution transcript profile across the wood-forming meristem of poplar identifies potential regulators of cambial stem cell identity. Plant Cell. 2004, 16: 2278-2292. 10.1105/tpc.104.024190.PubMedPubMed CentralView ArticleGoogle Scholar
- Paiva JA, Garnier-Gere PH, Rodrigues JC, Alves A, Santos S, Graca J, Le Provost G, Chaumeil G, Da Silva-Perez D, Bosc A, Fevereiro P, Plomion C: Plasticity of maritime pine (Pinus pinaster) wood-forming tissues during a growing season. New Phytol. 2008, 179: 1080-1094.PubMedView ArticleGoogle Scholar
- Plomion C, Leprovost G, Stokes A: Wood formation in trees. Plant Physiol. 2001, 127: 1513-1523. 10.1104/pp.010816.PubMedPubMed CentralView ArticleGoogle Scholar
- Zhang Y, Sederoff RR, Allona I: Differential expression of genes encoding cell wall proteins in vascular tissues from vertical and bent loblolly pine trees. Tree Physiol. 2000, 20: 457-466. 10.1093/treephys/20.7.457.PubMedView ArticleGoogle Scholar
- Hertzberg M, Aspeborg H, Schrader J, Andersson A, Erlandsson R, Blomqvist K, Bhalerao R, Uhlén M, Teeri T, Lundeberg J, Sundberg B, Nilsson P, Sandberg G: A transcriptional roadmap to wood formation. Proc Natl Acad Sci USA. 2001, 98: 14732-14737. 10.1073/pnas.261293398.PubMedPubMed CentralView ArticleGoogle Scholar
- Andersson-Gunnera S, Mellerowicz E, Love J, Segerman B, Ohmiya Y, Coutinho P, Nilsson P, Henrissat B, Moritz T, Sundberg B: Biosynthesis of cellulose-enriched tension wood in Populus: global analysis of transcripts and metabolites identifies biochemical and developmental regulators in secondary wall biosynthesis. Plant J. 2006, 45: 144-165. 10.1111/j.1365-313X.2005.02584.x.View ArticleGoogle Scholar
- Cato S, McMillan L, Donaldson L, Richardson T, Echt C, Gardner R: Wood formation from the base to the crown in Pinus radiata: gradients of tracheid wall thickness, wood density, radial growth rate and gene expression. Plant Mol Biol. 2006, 60: 565-581. 10.1007/s11103-005-5022-9.PubMedView ArticleGoogle Scholar
- Foucart C, Paux E, Ladouce N, San-Clemente H, Grima-Pettenati J, Sivadon P: Transcript profiling of a xylem vs phloem cDNA subtractive library identifies new genes expressed during xylogenesis in Eucalyptus. New Phytol. 2006, 170: 739-752. 10.1111/j.1469-8137.2006.01705.x.PubMedView ArticleGoogle Scholar
- Paiva JA, Garces M, Alves A, Garnier-Gere P, Rodrigues JC, Lalanne C, Porcon S, Le Provost G, Perez Dda S, Brach J, Frigerio JM, Claverol S, Barre A, Fevereiro P, Plomion C: Molecular and phenotypic profiling from the base to the crown in maritime pine wood-forming tissue. New Phytol. 2008, 178: 283-301. 10.1111/j.1469-8137.2008.02379.x.PubMedView ArticleGoogle Scholar
- Pavy N, Boyle B, Nelson C, Paule C, Giguere I, Caron S, Parsons LS, Dallaire N, Bedon F, Berube H, Cooke J, Mackay J: Identification of conserved core xylem gene sets: conifer cDNA microarray development, transcript profiling and computational analyses. New Phytol. 2008, 180: 766-786. 10.1111/j.1469-8137.2008.02615.x.PubMedView ArticleGoogle Scholar
- Boerjan W, Ralph J, Baucher M: Lignin biosynthesis. Annu Rev Plant Biol. 2003, 54: 519-546. 10.1146/annurev.arplant.54.031902.134938.PubMedView ArticleGoogle Scholar
- Aspeborg H, Schrader J, Coutinho P, Stam M, Kallas A, Djerbi S, Nilsson P, Denman S, Amini B, Sterky F, Master E, Sandberg G, Mellerowicz E, Sundberg B, Henrissat B, Teeri T: Carbohydrate-active enzymes involved in the secondary cell wall biogenesis in hybrid aspen. Plant Physiol. 2005, 137: 983-997. 10.1104/pp.104.055087.PubMedPubMed CentralView ArticleGoogle Scholar
- Vanholme R, Morreel K, Ralph J, Boerjan W: Lignin engineering. Curr Opin Plant Biol. 2008, 11: 278-285. 10.1016/j.pbi.2008.03.005.PubMedView ArticleGoogle Scholar
- Vander Mijnsbrugge K, Meyermans H, Van Montagu M, Bauw G, Boerjan W: Wood formation in poplar: identification, characterization, and seasonal variation of xylem proteins. Planta. 2000, 210: 589-598. 10.1007/s004250050048.PubMedView ArticleGoogle Scholar
- Whetten R, Sun Y-H, Zhang Y, Sederoff R: Functional genomics and cell wall biosynthesis in loblolly pine. Plant Mol Biol. 2001, 47: 275-291. 10.1023/A:1010652003395.PubMedView ArticleGoogle Scholar
- Shen B, Li C, Tarczynski M: High free-methionine and decreased lignin content result from a mutation in the Arabidopsis S-adenosyl-Lmethionine synthetase 3 gene. Plant J. 2002, 29: 371-380. 10.1046/j.1365-313X.2002.01221.x.PubMedView ArticleGoogle Scholar
- Sánchez-Aguayo I, Rodríguez-Galán J, García R, Torreblanca J, Pardo J: Salt stress enhances xylem development and expression of S-adenosyl-L-methionine synthase in lignifying tissues of tomato plants. Planta. 2004, 220: 278-285. 10.1007/s00425-004-1350-2.PubMedView ArticleGoogle Scholar
- Cantón F, Suárez M, Cánovas F: Molecular aspects of nitrogen mobilization and recycling in trees. Photosynth Res. 2005, 83: 265-278. 10.1007/s11120-004-9366-9.PubMedView ArticleGoogle Scholar
- Du S, Yamamoto F: An overview of the biology of reaction wood formation. J Integr Plant Biol. 2007, 49: 131-143. 10.1111/j.1744-7909.2007.00427.x.View ArticleGoogle Scholar
- Timell T: Compression wood in gymnosperms. 1986, Springer, HeidelbergView ArticleGoogle Scholar
- Donaldson L, Grace J, Downes G: Within-tree variation in anatomical properties of compression wood in radiata pine. IAWA Journal. 2004, 25: 253-271.View ArticleGoogle Scholar
- Sedighi-Gilani M, Sunderland H, Navi P: Microfibril angle non-uniformities within normal and compression wood tracheids. Wood Sci Technol. 2005, 39: 419-430. 10.1007/s00226-005-0022-0.View ArticleGoogle Scholar
- Önnerud H: Lignin structures in normal and compression wood. Evaluation by thioacidolysis using ethanethiol and methanethiol. Holzforschung. 2003, 57: 377-384.Google Scholar
- Yeh T-F, Goldfarb B, Chang H-, Peszlen I, Braun J, Kadla J: Comparison of morphological and chemical properties between juvenile wood and compression wood of loblolly pine. Holzforschung. 2005, 59: 669-674.View ArticleGoogle Scholar
- Allona I, Quinn M, Shoop E, Swope K, St Cyr S, Carlis J, Riedl J, Retzel E, Campbell MM, Sederoff R, Whetten RW: Analysis of xylem formation in pine by cDNA sequencing. Proc Natl Acad Sci USA. 1998, 95: 9693-9698. 10.1073/pnas.95.16.9693.PubMedPubMed CentralView ArticleGoogle Scholar
- Pavy N, Laroche J, Bousquet J, Mackay J: Large-scale statistical analysis of secondary xylem ESTs in pine. Plant Mol Biol. 2005, 57: 203-224. 10.1007/s11103-004-6969-7.PubMedView ArticleGoogle Scholar
- Yamashita S, Yoshida M, Yamamoto H, Okuyama T: Screening genes that change expression during compression wood formation in Chamaecyparis obtusa. Tree Physiol. 2008, 28: 1331-1340. 10.1093/treephys/28.9.1331.PubMedView ArticleGoogle Scholar
- Yeh T-F, Braun J, Goldfarb B, Chang H-, Kadla J: Morphological and chemical variations between juvenile wood, mature wood, and compression wood of loblolly pine (Pinus taeda L.). Holzforschung. 2006, 60: 1-8.View ArticleGoogle Scholar
- Yeh TF, Morris CR, Goldfarb B, Chang HM, Kadla JF: Utilization of polar metabolite profiling in the comparison of juvenile wood and compression wood in loblolly pine (Pinus taeda). Tree Physiol. 2006, 26: 1497-1503. 10.1093/treephys/26.11.1497.PubMedView ArticleGoogle Scholar
- Alía R, Martín S, Miguel JD, Galera R, Agúndez D, Gordo J, Salvador L, Catalán G,Gil L: Las regions de procedencia de Pinus pinaster Aiton. Madrid: DGCONA; 1996.Google Scholar
- Cantón F, Provost GL, Garcia V, Barré A, Frigério J, Paiva J, Fevereiro P, Avila C, Mouret J, Daruvar AD, Cánovas F, Plomion C: Transcriptome analysis of wood formation in maritime pine. Sustainable forestry, wood products & biotechnology. Edited by: Espinel S, Barredo Y, Ritter E. 2003, DFA-AFA Press, Vitoria-Gasteiz, Spain, 334-347.Google Scholar
- Altschul SF, Gish W, Miller W, Myers EW, Lipman DJ: Basic local alignment search tool. J Mol Biol. 1990, 215: 403-410.PubMedView ArticleGoogle Scholar
- Roje S: S-Adenosyl-L-methionine: beyond the universal methyl group donor. Phytochemistry. 2006, 67: 1686-1698. 10.1016/j.phytochem.2006.04.019.PubMedView ArticleGoogle Scholar
- Avila C, Suarez M, Gomez-Maldonado J, Canovas F: Spatial and temporal expression of two cytosolic glutamine synthetase genes in Scots pine: functional implications on nitrogen metabolism during early stages of conifer development. Plant J. 2001, 25: 93-102. 10.1046/j.1365-313x.2001.00938.x.PubMedView ArticleGoogle Scholar
- Davin L, Lewis N: An historical perspective on lignan biosynthesis: monolignol, allylphenol and hydroxycinnamic acid coupling and downstream metabolism. Phytochem Rev. 2003, 2: 257-288.View ArticleGoogle Scholar
- Kasahara H, Jiao Y, Bedgar D, Kim S-J, Patten A, Xia Z-Q, Davin L, Lewis N: Pinus taeda phenylpropenal double-bond reductase: purification, cDNA cloning, heterologous expression in Escherichia coli, and subcellular localization in P. taeda. Phytochemistry. 2006, 67: 1765-1780. 10.1016/j.phytochem.2006.07.001.PubMedView ArticleGoogle Scholar
- Lohrasebi H, Mabee W, Roy D: Chemistry and pulping feasibility of compression wood in black spruce. J Wood Chem and Technol. 1999, 19: 13-25. 10.1080/02773819909349597.View ArticleGoogle Scholar
- Spokevicius AV, Southerton SG, MacMillan CP, Qiu D, Gan S, Tibbits JF, Moran GF, Bossinger G: Beta-tubulin affects cellulose microfibril orientation in plant secondary fibre cell walls. Plant J. 2007, 51: 717-726. 10.1111/j.1365-313X.2007.03176.x.PubMedView ArticleGoogle Scholar
- Wightman R, Turner SR: The roles of the cytoskeleton during cellulose deposition at the secondary cell wall. Plant J. 2008, 54: 794-805. 10.1111/j.1365-313X.2008.03444.x.PubMedView ArticleGoogle Scholar
- Hamada T: Microtubule-associated proteins in higher plants. J Plant Res. 2007, 120: 79-98. 10.1007/s10265-006-0057-9.PubMedView ArticleGoogle Scholar
- Zhong R, Burk DH, Morrison WH, Ye ZH: A kinesin-like protein is essential for oriented deposition of cellulose microfibrils and cell wall strength. Plant Cell. 2002, 14: 3101-3117. 10.1105/tpc.005801.PubMedPubMed CentralView ArticleGoogle Scholar
- Burk DH, Ye ZH: Alteration of oriented deposition of cellulose microfibrils by mutation of a katanin-like microtubule-severing protein. Plant Cell. 2002, 14: 2145-2160. 10.1105/tpc.003947.PubMedPubMed CentralView ArticleGoogle Scholar
- Pesquet E, Korolev AV, Calder G, Lloyd CW: The microtubule-associated protein AtMAP70-5 regulates secondary wall patterning in Arabidopsis wood cells. Curr Biol. 2010, 20: 744-749. 10.1016/j.cub.2010.02.057.PubMedView ArticleGoogle Scholar
- Treacy M, Evertsen J, Dhubháin AN: A comparison of mechanical andphysical wood properties of a range of sitka spruce provenances. Dublin:National Council for Forest Research and Development (COFORD); 2000.Google Scholar
- Bourquin V, Nishikubo N, Abe H, Brumer H, Denman S, Eklund M, Christiernin M, Teeri T, Sundberg B, Mellerowicz E: Xyloglucan endotransglycosylases have a function during the formation of secondary cell walls of vascular tissues. Plant Cell. 2002, 14: 3073-3088. 10.1105/tpc.007773.PubMedPubMed CentralView ArticleGoogle Scholar
- Broeck H, Maliepaard C, Ebskamp M, Toonen MAJ, Koops AJ: Differential expression of genes involved in C1 metabolism and lignin biosynthesis in wooden core and bast tissues of fibre hemp (Cannabis sativa L.). Plant Sci. 2008, 174: 205-220. 10.1016/j.plantsci.2007.11.008.View ArticleGoogle Scholar
- Mouillon J-M, Aubert S, Bourguignon J, Gout E, Douce R, Rébeillé F: Glycine and serine catabolism in non-photosynthetic higher plant cells: their role in C1 metabolism. Plant J. 1999, 20: 197-205. 10.1046/j.1365-313x.1999.00591.x.PubMedView ArticleGoogle Scholar
- Douce R, Bourguignon J, Neuburger M, Rébeillé F: The glycine decarboxylase system: a fascinating complex. Trends Plant Sci. 2001, 6: 167-176. 10.1016/S1360-1385(01)01892-1.PubMedView ArticleGoogle Scholar
- Rajinikanth M, Harding S, Tsai C-J: The glycine decarboxylase complex multienzyme family in Populus. J Exp Bot. 2007, 58: 1761-1770. 10.1093/jxb/erm034.PubMedView ArticleGoogle Scholar
- Ho C-L, Saito K: Molecular biology of the plastidic phosphorylated serine biosynthetic pathway in Arabidopsis thaliana. Amino Acids. 2001, 20: 243-259. 10.1007/s007260170042.PubMedView ArticleGoogle Scholar
- Fell D: Increasing the flux in metabolic pathways: a metabolic control analysis perspective. Biotechnol Bioeng. 1998, 58: 121-124. 10.1002/(SICI)1097-0290(19980420)58:2/3<121::AID-BIT2>3.0.CO;2-N.PubMedView ArticleGoogle Scholar
- Miyazaki J, Yang S: The methionine salvage pathway in relation to ethylene and polyamine biosynthesis. Physiol Plant. 1987, 69: 366-370. 10.1111/j.1399-3054.1987.tb04302.x.View ArticleGoogle Scholar
- Canovas FM, Avila C, Canton FR, Canas RA, de la Torre F: Ammonium assimilation and amino acid metabolism in conifers. J Exp Bot. 2007, 58: 2307-2318. 10.1093/jxb/erm051.PubMedView ArticleGoogle Scholar
- Vander Mijnsbrugge K, Beeckman H, De Rycke R, Van Montagu M, Engler G, Boerjan W: Phenylcoumaran benzylic ether reductase, a prominent poplar xylem protein, is strongly associated with phenylpropanoid biosynthesis in lignifying cells. Planta. 2000, 211: 502-509. 10.1007/s004250000326.PubMedView ArticleGoogle Scholar
- Möller R, McDonald A, Walter C, Harris P: Cell differentiation, secondary cell-wall formation and transformation of callus tissue of Pinus radiata D. Don. Planta. 2003, 217: 736-747. 10.1007/s00425-003-1053-0.PubMedView ArticleGoogle Scholar
- Regan S, Bourquin V, Tuominen H, Sundberg B: Accurate and high resolution in situ hybridization analysis of gene expression in secondary stem tissues. Plant J. 1999, 19: 363-369. 10.1046/j.1365-313X.1999.00536.x.PubMedView ArticleGoogle Scholar
- Canas RA, de la Torre F, Canovas FM, Canton FR: Coordination of PsAS1 and PsASPG expression controls timing of re-allocated N utilization in hypocotyls of pine seedlings. Planta. 2007, 225: 1205-1219. 10.1007/s00425-006-0431-9.PubMedView ArticleGoogle Scholar
- Lange B, Lapierre C, Sandermann H: Elicitor-induced spruce stress lignin. Plant Physiol. 1995, 108: 1277-1287.PubMedPubMed CentralGoogle Scholar
- Chang S, Puryear J, Cairney J: A simple and efficient method for isolating RNA from pine tree. Plant Mol Biol Rep. 1993, 11: 113-116. 10.1007/BF02670468.View ArticleGoogle Scholar
- Yang YH, Dudoit S, Luu P, Lin DM, Peng V, Ngai J, Speed TP: Normalization for cDNA microarray data: a robust composite method addressing single and multiple slide systematic variation. Nucleic Acids Res. 2002, 30: e15-10.1093/nar/30.4.e15.PubMedPubMed CentralView ArticleGoogle Scholar
- Smyth G: Linear models and empirical bayes methods for assesing differential expression in microarray experiments. Stat Appl Genet Mol Biol. 2004, 3: 1-26.Google Scholar
- Benjamini Y, Hochberg Y: Controlling the false discovery rate: a practical and powerful approach to multiple testing. J R Statist Soc B. 1995, 57: 289-300.Google Scholar
- Gentleman RC, Carey VJ, Bates DM, Bolstad B, Dettling M, Dudoit S, Ellis B, Gautier L, Ge Y, Gentry J, Hornik K, Hothorn T, Huber W, Iacus S, Irizarry R, Leisch F, Li C, Maechler M, Rossini AJ, Sawitzki G, Smith C, Smyth G, Tierney L, Yang JY, Zhang J: Bioconductor: open software development for computational biology and bioinformatics. Genome Biol. 2004, 5: R80-10.1186/gb-2004-5-10-r80.PubMedPubMed CentralView ArticleGoogle Scholar
- Smyth G: Limma: linear models for microarray data. In Bioinformatics andcomputational biology solutions using R and Bioconductor. Edited byGentleman R, Carey V, Dudoit S, Irizarry R, Huber W. New York: Springer;2005:397–420.View ArticleGoogle Scholar
- Falgueras J, Lara AJ, Fernandez-Pozo N, Canton FR, Perez-Trabado G, Claros MG: SeqTrim: a high-throughput pipeline for pre-processing any type of sequence read. BMC Bioinformatics. 2010, 11: 38-10.1186/1471-2105-11-38.PubMedPubMed CentralView ArticleGoogle Scholar
- Huang X, Madan A: CAP3: a DNA sequence assembly program. Genome Res. 1999, 9: 868-877. 10.1101/gr.9.9.868.PubMedPubMed CentralView ArticleGoogle Scholar
- Ruepp A, Zollner A, Maier D, Albermann K, Hani J, Mokrejs M, Tetko I, Guldener U, Mannhaupt G, Munsterkotter M, Mewes HW: The FunCat, a functional annotation scheme for systematic classification of proteins from whole genomes. Nucleic Acids Res. 2004, 32: 5539-5545. 10.1093/nar/gkh894.PubMedPubMed CentralView ArticleGoogle Scholar
- Cantón FR, Quail PH: Both phyA and phyB mediate light-imposed repression of PHYA gene expression in Arabidopsis. Plant Physiol. 1999, 121: 1207-1216. 10.1104/pp.121.4.1207.PubMedPubMed CentralView ArticleGoogle Scholar
- Zhao S, Fernald RD: Comprehensive algorithm for quantitative real-time polymerase chain reaction. J Comput Biol. 2005, 12: 1047-1064. 10.1089/cmb.2005.12.1047.PubMedPubMed CentralView ArticleGoogle Scholar
- Vandesompele J, De Preter K, Pattyn F, Poppe B, Van Roy N, De Paepe A, Speleman F: Accurate normalization of real-time quantitative RT-PCR data by geometric averaging of multiple internal control genes. Genome Biol. 2002, 3: R34.View ArticleGoogle Scholar
This article is published under license to BioMed Central Ltd. This is an Open Access article distributed under the terms of the Creative Commons Attribution License (http://creativecommons.org/licenses/by/2.0), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.