Lignocellulosic biomass has potential as an abundant and renewable feedstock for biofuel production. The main component of lignocellulosic biomass is the secondary walls of plant cells. A need for dedicated bioenergy crops with improved cell wall compositions and properties has become evident if biofuels are to be a cost-efficient alternative to fossil fuels [1, 2].

Secondary cell walls of plants consist of cellulose microfibrils embedded in a matrix consisting mainly of hemicelluloses and lignin, the amounts of each single polymer varying widely between different species and cell types. Together these complex sugar polymers form rigid barriers that provide shape, structural strength and protection against environmental stresses and pathogens [24]. Hemicelluloses – mainly xylans – make up 20-35% of the secondary cell wall. In grasses, xylans are also the main noncellulosic polysaccharide in the primary walls [2, 4, 5]. As such, xylans represent a major part of the available biomass.

The bioconversion of lignocellulosic biomass into biofuels is currently suffering under the considerable recalcitrance of the biomass toward efficient deconstruction processes of the polymers into simple sugars [1, 6]. Hemicelluloses and lignin embed cellulose microfibrils in a tight matrix, thus hindering access of cell wall degrading enzymes to the polysaccharides [7, 8]. In addition, xylans are composed almost entirely of pentose sugars, which cannot be efficiently fermented [9, 10]. Finally, xylans are heavily esterified with acetate, especially in hardwoods, and this hinders efficient enzymatic hydrolysis while the released acetate inhibits yeast fermentations [11, 12]. For all these reasons, plants that have reduced amounts of xylan in their secondary cell walls, while still maintaining normal growth and development, would present a valuable feedstock for biofuel production.

Xylans are polysaccharides that have linear backbones of β-(1→4)-linked d-xylosyl residues that can be substituted with various side chains. The major xylan in dicot plants, glucuronoxylan (GX), is decorated with side chains of α-d-glucuronic acid (GlcA) and 4-O-methyl-α-d-glucuronic acid (MeGlcA). Moreover, acetylation is especially common in the secondary walls of this group of plants [5]. GXs from angiosperm and gymnosperm species have been shown to contain a reducing end oligosaccharide sequence consisting of β-d-Xylp-(1→4)-β-d-Xylp-(1→3)-α-l-Rhap-(1→2)-α-d-Galp A-(1→4)-d-Xylp[1315]. The reducing end oligosaccharide has so far not been detected in grasses. It is not known whether this oligosaccharide functions as a primer for xylan biosynthesis or as a terminator sequence [15, 16].

While the biosynthesis of other hemicelluloses with β-(1→4)-linked backbones involves the Cellulose Synthase Like (CSL) protein families, this does not appear to be the case for xylans [4, 17]. Studies mostly of Arabidopsis mutants have led to the identification of several glycosyltransferases (GTs) with a role in xylan biosynthesis: IRX9/IRX9L [18] and IRX14/IRX14L [18, 19] from GT family GT43 as well as IRX10/IRX10L [20, 21] from GT47 seem to be involved in biosynthesis of the xylan backbone, while IRX8 (GAUT12) [15] and PARVUS (GATL1) [15, 22] from GT8 and IRX7 (FRA8) and IRX7L (F8H) [23, 24] from GT47 may be involved in synthesizing the reducing end oligosaccharide. All these GTs are predicted to be Golgi-localized type II membrane proteins. None of the proteins have had their biochemical activity determined and it is therefore not clear how they work together in the biosynthesis of xylan, but some studies indicate that they may function in protein complexes [25, 26].

The GTs responsible for adding substitutions to xylan are better understood. Enzymes from GT61 are responsible for adding arabinosyl residues to the xylan backbone [27], and other enzymes from GT61 add xylose to such arabinosyl residues in grasses [28]. The glucuronosyl residues are added by GlucUronic acid substitution of Xylan (GUX) enzymes that belong to GT8 [2931], and methyl groups are added to the glucuronic acid residues by a methyltransferase belonging to the DUF579 family [32].

The irregular xylem 7 (irx7), irx8 and irx9 T-DNA insertion mutants are deficient in GX biosynthesis, the resultant phenotype being the characteristic irregular xylems that arise when the weakened xylem vessels collapse inward, as they can no longer withstand the negative pressure that allows water to travel through the vessels. The irx7, irx8, and irx9 Arabidopsis mutants have severely dwarfed whole plant morphologies and are largely infertile [33]. For both IRX7 and IRX9, there are redundant genes, IRX7L and IRX9L, respectively, which are not highly expressed in tissues with secondary walls, but still influence the phenotype. The double knock-out mutations irx7/irx7L and irx9/irx9L are essentially lethal [18]. Different alleles have been described for irx9 and the irx9-2 mutant has a milder growth phenotype with a less severely stunted growth than the irx9-1 mutant and remains fertile [15, 18, 34]. Through analyses of the irx7, irx8 and irx9 mutants, it was found that they are specifically expressed in developing vascular tissues where secondary walls are being deposited and are important for wall thickness and integrity. Xylose content in irx7, irx8 and irx9 is 28%, 35% and 45% less than wild type levels, respectively, and the mutants have significant reductions in cellulose content that is thought to be a consequence of the stunted growth of the plants and not a direct effect of the lost gene function. Together, these deficiencies cause large reductions in wall thickness of ~60% in all three mutants [15, 3335]. As the wall integrity is compromised in irx7, irx8 and irx9, the mechanical breaking force of the stems is considerably lower than that of wild type plants [15, 35]. In irx7 and irx8, the reducing end oligosaccharide is largely absent, and they show a decrease in the number of GX chains. In contrast, the reducing end oligosaccharide is retained in the irx9 mutant while the number of GX chains is increased and the chain length is decreased [15, 34, 35]. All these mutants retain substitution with MeGlcA but are devoid of GlcA substitution.

The spatial, temporal and quantitative expression of genes is controlled by transcription factors. The regulation of cell wall polysaccharide biosynthesis has been shown to involve a complex network of transcription factors, several of which are members of the plant specific NAC (N AM, A TAF1/2 and C UC2) domain proteins [3638]. Vascular-related NAC Domain 6 (VND6) (At5g62380) and VND7 (At1g71930), together with the closely related NAC Secondary Wall Thickening Promoting Factor 1 (NST1) and NST3 (SND1) transcription factors, have been shown to be key regulatory switches for activation of secondary cell wall biosynthesis. VND6/VND7 and NST1/NST3 separately and/or collectively activate the biosynthetic pathways for cellulose, xylan and lignin through activation of a cascade of direct and indirect downstream transcription factors, many of which belong to the MYB family of transcription factors [3942].These master regulators exhibit cell specific expression patterns, where VND6 and VND7 specifically regulate secondary cell wall biosynthesis in vessels while expression of NST1 and NST3 is confined to fibers [4348]. VND6 and VND7 show vascular-specific expression patterns, the expression of VND6 being specifically located in the inner-metaxylem vessels, while that of VND7 is present in the protoxylem poles of the procambium region and in differentiating protoxylem and metaxylem vessels [43, 49, 50]. The function of VND6 and VND7 genes as key regulators of xylem vessel development was illustrated when they were overexpressed under the control of the cauliflower mosaic virus 35S promoter [43]. This experiment showed that various cell types could be transdifferentiated into xylem vessel elements with reticulated or pitted patterns like those of the metaxylem for the VND6 construct, and into xylem vessels with annular or spiral patterns like those of protoxylem vessels for the VND7 construct. Furthermore, dominant repression of either gene by fusion to the SRDX-domain specifically inhibited metaxylem and protoxylem formation, respectively [43].

The morphological effect of the irx mutations led us to hypothesize that the main reason for dwarfed growth in irx mutants is the collapsed vessels, and that specifically restoring xylan biosynthesis in vessels would therefore complement the mutations (Figure 1). We used Arabidopsis irx7, irx8 and irx9 mutants as backgrounds with strongly reduced amounts of GX in the secondary walls to reintroduce GX synthesis specifically in the vascular tissues, by exploiting the tissue-specific expression patterns of the VND6 and VND7 promoters. The dwarfed growth and irx-phenotype of the irx7, irx8 and irx9 mutants could be complemented to varying degrees, in some cases completely restoring wild-type growth patterns and mechanical properties while maintaining a low overall xylan content and improved saccharification properties.

Figure 1
figure 1

Model of engineering strategy. The xylan engineering strategy reintroduces xylan biosynthesis specifically into the xylem vessels of the xylan deficient irx7, irx8 and irx9 mutants. This is achieved through the expression of a functional allele of the defective irx gene under control of the vessel-specific pVND6 or pVND7 promoters.


Vessel specific expression of the IRX7, IRX8 and IRX9 genes in the irx7, irx8 and irx9 mutant plants

T-DNA insertional mutants in IRX7, IRX8 and IRX9 were used as genetic backgrounds for the xylan engineering (see Figure 2). The first attempt to engineer plants with decreased xylan content focused on the irx9-2 (from here on referred to as irx9) mutant, which has the advantage of being fertile and transformable, in contrast to the irx7 and irx8-6 (from here on referred to as irx8) mutants. Thus, homozygous irx9 plants were used for transformation with Agrobacterium tumefaciens (Agrobacterium) containing the pVND6:IRX9 and pVND7:IRX9 constructs. Due to the severely affected growth of the irx7 and irx8 mutants, plants homozygous for their respective defective irx allele have poor fertility [33, 34]. For transformation of the irx7 mutant with the pVND6:IRX7 and pVND7:IRX7 constructs, and of the irx8 mutant with the pVND6:IRX8 and pVND7:IRX8 constructs, we selected plant lines that were heterozygous for the defective irx7 and irx8 allele, respectively. For each of the plant lines, positive T1 transformants were identified by screening for hygromycin resistance. Positive transformants in irx7 and irx8 backgrounds were also genotyped to identify hygromycin resistant plants that were homozygous for the defective irx allele. Plant lines with the best growth indicating good complementation of the irx phenotype were chosen for further analysis in T2. Prior to analysis of growth and cell wall properties, the selected plant lines were analyzed by PCR to confirm the presence of the respective transgene and by RT-PCR to ensure that the transgene was expressed (Figure 3).

Figure 2
figure 2

Schematic illustration of the IRX genes and T-DNA insertions for the irx mutants. (A) irx9-2 in At2g37090 (IRX9) is located in the coding region of an exon. (B) irx8-6 in At5g54690 (IRX8) is located in an intron. (C) irx7 in At2g28110 (IRX7) is located in a non-coding region of an exon. T-DNAs are indicated with triangles.

Figure 3
figure 3

Detection of transgene presence and expression. (A) Agarose gels showing the presence of the transgene by PCR. Leaves from 6-week old plants were used. (B) RT-PCR analysis confirming expression of IRX7 and IRX9 genes respectively in stems of transformed plants. Actin2 was amplified as control. cDNA was prepared from stems (top 5 cm) of 6-week old plants.

Growth complementation of rosettes and inflorescence stems

Weekly measurements of the growth of rosettes and inflorescence stems were conducted for the irx mutants transformed with the respective pVND6 and pVND7 constructs, along with the wild type and the irx7, irx8, and irx9 mutants (Figures 4 and 5). The irx7, irx8 and irx9 mutants showed the characteristic dwarfed phenotype and smaller, dark green leaves previously described [33]. The morphology of irx9 transformants containing the pVND7:IRX9 construct (Figure 4A and B) resembled that of the wild type at the rosette stage, but had a mildly stunted growth of the inflorescence stem compared to that of the wild type. Transformation with the pVND6:IRX9 construct (Figure 4A and B) yielded plants with a morphology that looked more similar to that of irx9 mutants. The rosettes of pVND6:IRX7, pVND6:IRX8 and pVND7:IRX8 (Figure 5A and B) transformants were smaller than those of the wild-type plants, while their inflorescence stems were intermediate in size between the wild type and their corresponding irx mutants (Figure 5A and C). In contrast, the irx7 mutants harboring pVND7:IRX7 (Figure 5) grew similarly to the wild type in respect to both rosette and stem growth, suggesting that the irx phenotype may be fully complemented in these transformants.

Figure 4
figure 4

Representative morphological phenotypes of plants showing growth complementation of the irx9 mutant. (A) Scale bars: 10 mm. (B) The graph shows average diameter of the rosettes ± SE (n=5 for wild type, n=4 for pVND6:IRX9 lines, n=7 for pVND7:IRX9 #1, and n=6 for pVND7:IRX9 #5).

Figure 5
figure 5

Representative morphological phenotypes of plants showing growth complementation of the irx7 and irx8 mutants. (A) Scale bars: 10 mm. (B) Average diameter of rosettes ± SE (n= 6); (C) Average height of the inflorescence stem ± SE (n=6). Bars that are not labeled with the same letter represent significantly different values (t-test, p < 0.05).

Microscopic analysis of the pVND6/pVND7:IRX7/IRX8/IRX9 expressing transformants

The effect of the pVND6/pVND7:IRX7/IRX8/IRX9 constructs on vascular tissue morphology was examined by analysis of transverse sections of the lower parts of inflorescence stems. Xylem vessels of wild type plants are characterized by large open cells that are relatively round in shape, while the interfascicular fibers are heavily lignified (Figure 6A) [51]. The xylem vessels of irx7, irx8 and irx9 are often smaller in size and have irregular shapes caused by large reductions in wall thickness (Figures 6B, 7B and E) [33].

Figure 6
figure 6

Tissue analysis of stems in irx9 transformant lines. (A1-D1) Immunodetection of xylan in transverse stem sections with the LM10 anti-xylan monoclonal antibody (A2-D2) Lignin deposition in the secondary walls was stained with Phloroglucinol-HCl. (A3-D3) Same as A2-D2, at higher magnification; arrows point to some of the irregular xylem cells. Scale bars for all panels: 100 μm.

Figure 7
figure 7

Tissue analysis of stems in irx7 and irx8 transformant lines. (A1-G1) Immunodetection of xylan in transverse stem sections with the LM10 anti-xylan monoclonal antibody. (A2-G2) Lignin deposition in the secondary walls was stained with Phloroglucinol-HCl. (A3-G3) Same as A2-G2, at higher magnification; arrows point to some of the irregular xylem cells. Scale bars for all panels: 100 μm.

Stem sections were immunolabeled with the LM10 monoclonal antibody to examine xylan distribution in the cell wall. The antibody recognizes unsubstituted and lowly substituted β-(1→4)-xylans [52] and its epitope has been shown to be specifically associated with cell types with secondary cell walls in Arabidopsis stems [53]. In the irx mutants, the decreased GX content resulted in a lower intensity of fluorescence in the xylem and interfascicular fibers when compared to the wild type sections.

Expression of IRX9 under the control of the pVND6 or pVND7 promoter did not rescue the collapsed xylem vessels of the irx9 mutant to a noticeable degree (Figure 6C and D). The pVND6:IRX7, pVND6:IRX8 and pVND7:IRX8 transformants had slightly less collapsed xylem cells compared to their respective irx mutant backgrounds, but still retained the thin cell walls in both xylem vessels and interfascicular fibers (Figure 7C, F, and G). In contrast, the pVND7:IRX7 transformants showed large open vessels that were comparable to those of the wild type (Figure 7D). The fluorescence intensity of the xylem vessels and the interfascicular fibers of pVND7:IRX7 plants resembled those of irx7, indicating reduced overall amounts of xylan compared to the wild type (Figure 7D).

The phloroglucinol-HCl stain was used to visualize lignin depositions in the cell walls [54]. Wild type stem sections showed thick lignified cell walls in both the vessels and interfascicular fibers. The irx9 mutant contained wild type-like levels of lignin in the xylem vessels and reduced amounts in the interfascicular fibers (Figure 6B2-3). The relatively large degree of lignification in irx9 may account for the less severe growth phenotype of this mutant. Lignin deposition in the pVND6/pVND7:IRX9 transformants was comparable to that of the wild type in the xylem vessels and to irx9 in the interfascicular fibers, however the xylem vessels were still collapsed (Figure 6C2 and D2). In contrast, irx7 and irx8 mutant plants have very low levels of lignification in both the xylem vessels and interfascicular fibers (Figure 7B2-3 and E2-3). In the pVND6:IRX7 transformants lignin deposition was comparable to that of the irx7 mutant (Figure 7C2). The pVND6:IRX8 transformants exhibited similar amounts of lignin to those of wild type in the xylem cells and in the interfascicular fibers (Figure 7F2-3), while lignification in the pVND7:IRX8 transformants was intermediate between that of irx8 and wild type in both cell types (Figure 7G2-3). In the pVND7:IRX7 lines lignification was almost completely restored in both xylem cells and interfascicular fibers (Figure 7D2-3).

Analysis of cell wall composition

Monosaccharide compositional analysis after hydrolysis with TFA was performed on cell wall preparations from the basal part of the inflorescence stem. This analysis demonstrated that xylose contents in all transformants were reduced to levels resembling that of the respective irx mutant or to intermediate levels between that of the mutant and the wild type (Figure 8A and B). Cell wall monosaccharide analysis of the irx9 mutant transformed with the pVND7:IRX9 construct (Figure 8A) revealed a significant 17% reduction in xylose content compared to the wild type, while the irx7 transformants containing the pVND7:IRX7 construct (Figure 7B) showed significant reductions between 16-23% compared to the wild type. An overall increase for all other monosaccharides could be observed corresponding to the decrease in xylose.

Figure 8
figure 8

Monosaccharide composition of the cell wall from irx9, irx7 and irx8 plants transformed with IRX9 , IRX7 and IRX8 under the native VND6 and VND7 promoter. Cell wall material (alcohol insoluble residue, AIR) was prepared from fresh stem material, hydrolyzed with trifluoroacetic acid (A and B) or sulfuric acid (C), and analyzed by high-performance anion exchange chromatography. (A) All irx9 transformant lines have significantly reduced xylose content that are similar to those of the irx9 mutant. (B) The irx7 and irx8 transformant lines have intermediary xylose levels compared to the wild type and their respective irx7/irx8 backgrounds. (C) Hexose/pentose ratio in cell walls of transformed irx9 plants. The sugar content in the cell walls was determined after complete hydrolysis with sulfuric acid. All graphs show average ± SD (where (A) and (B) n=4 and (C) n=3) except for irx7 and irx8 mutants where only one replicate was available. * indicates a significant difference in xylose or C6/C5 ratio from the wild type (t-test, p < 0.01).

Transformants in the irx9 background were additionally subjected to analysis of total wall monosaccharide composition after hydrolysis with sulfuric acid, in order to calculate the ratio between total C6 and C5 sugars in the wall (Figure 8C). Transformants expressing the pVND6:IRX9 or the pVND7:IRX9 constructs exhibited a ratio of C6/C5 sugars that was increased up to 46% compared to the wild type, which is a ratio similar to that of the irx9 mutant.

Stem breaking-force measurements

To test the physical properties of the transformed plants, we performed breaking-force measurements on stem sections of 7-week-old plants (Figure 9). As expected, the irx9 mutant had a strongly reduced tensile strength compared to the wild type, and transformation with the pVND7:IRX9 constructs only partially restored the stem strength while transformants with the pVND6:IRX9 constructs were as weak as the irx9 mutant. Transformants of the irx7 mutant all showed significant recovery of stem strength. For the irx7 mutant transformed with the pVND6:IRX7 construct (line #44) stem strength was the same as in the wild type, and in line #55 with the pVND7:IRX7 construct stem strength even exceeded that of the wild type by 30% (Figure 9). The irx8 mutant transformed with the pVND6:IRX8 constructs also exhibited stem strength comparable to the wild type. Generally, the degree of recovery of stem strength was consistent with the recovery of growth and stem morphology discussed above (Figures 4, 5, 6, and 7).

Figure 9
figure 9

Breaking-force measurements of inflorescence stems. The tensile breaking strength of the main inflorescence stem of 7-week-old plants was tested. Values show average ± SD (n=5-9) of log-transformed data. * indicates a significant difference from the wild type (t-test, p < 0.05).

Quantification of lignin content

Due to the reduction in lignin content observed with the phloroglucinol-HCl staining method of inflorescence stem sections, we quantified the content of lignin in the transformed plants with the acetyl bromide assay. Transformants of irx9 harboring the pVND6/ pVND7:IRX9 constructs showed a 14-17% reduction in lignin content compared to the wild type (Figure 10A). Transformants in the irx7 background harboring the pVND6:IRX7 construct had a significantly lower lignin content compared to the wild type, whereas the other transformants in irx7 and irx8 mutant backgrounds did not show significant changes in lignin content (Figure 10B).

Figure 10
figure 10

Lignin quantification. (A) irx9 transformed lines. (n=3) (B) irx7 and irx8 transformed lines (n=4). Dry material from senesced stems was used for this analysis. Values show average ± SD. * indicates a significant difference from the wild type (t-test, p < 0.05).

Improvement in sugar release after saccharification

Upon hot water pretreatment and after 24 h of enzyme digestion with the Cellic CTec2 enzyme cocktail, all irx transformant lines showed an increase in saccharification yield compared to that of the wild type (Figure 11A). The pVND6/ pVND7:IRX9x lines showed improved saccharification yields of up to 55%, while the pVND6:IRX7 and pVND7:IRX7 lines showed improved yields of up to 49% and 42%, respectively. The released sugars from the two pVND7:IRX9 and three pVND7:IRX7 lines were further analyzed by HPAEC (Figure 11B). Clearly, the Cellic CTec2 enzyme mixture was most efficient in releasing glucose, with a much less efficient release of xylose. The irx9 mutant and the transformants all showed an increased release in glucose. However, it is not possible to conclude if this increase is due to better accessibility to cellulose or simply reflects that the biomass has relatively higher cellulose content. The irx9 mutant and pVND7:IRX9 lines also showed increased release of xylose, which is somewhat surprising given that these lines have lower xylan content. This suggests that xylan is more accessible to enzymatic breakdown in these lines and may be explained by their lower lignin content (Figure 10B). In contrast, the pVND7:IRX7 lines which did not show an increased xylan release (Figure 11B) had normal lignin content (Figure 10B).

Figure 11
figure 11

Saccharification analysis. Hot water pretreatment of dry stem material was followed by 24 h of saccharification with the Cellic CTec2 (Novozymes) enzyme mixture. (A) Release of reducing sugar was determined by the dinitrosalicylic acid assay. All transformants showed increases in saccharification yield compared to the wild type. Values show average ± SD (n=7 for wild type, irx9 mutant and pVND7:IRX9 #5, both pVND6:IRX9 lines and pVND7:IRX9 #1 n=3, and all remaining lines n=4). (B) Released sugars from selected lines were analyzed by HPAEC. Values show average ± SE (n = 3 for wild type and irx9, and n=8 for pVND7:IRX9 and pVND7:IRX7 lines). Fucose, rhamnose, arabinose and galactose were present in trace amounts. * indicates a significant difference from the wild type (t-test, p < 0.05).


Complementation of the irx7, irx8 and irx9 growth phenotypes through vessel-specific expression of IRX7, IRX8, and IRX9

The irx7, irx8 and irx9 mutants have large reductions in GX content, a trait that increases saccharification yields considerably, but also reduces total biomass yields through severely impaired growth of the plants [7, 8, 33]. The phenotype of these and other mutants affected in xylan biosynthesis has demonstrated that xylans are essential polysaccharides in plant cell walls. However, the results presented here show that while xylans are essential for plants, they are not essential in all cell types. Indeed, the stunted growth of the irx mutants appears to be caused predominantly by collapsed xylem vessels and subsequent impaired nutrient and water transport. Consequently, we could alleviate the growth phenotype and still retain the low xylan levels of the irx mutants by an engineering approach that enables the re-introduction of xylan biosynthesis specifically in the xylem vessels of xylan deficient irx mutants.

Expression of the wild type IRX7, IRX8 and IRX9 cDNAs under control of the pVND6 or pVND7 promoter in the respective irx7, irx8 and irx9 mutant backgrounds yielded improved growth patterns of both rosette size and stem height for all transformant lines, when compared to the respective irx mutant (Figures 4 and 5). As expected, individual lines showed variation in the degree of growth complementation. However, overall there were some general patterns found. For both the irx7 and irx9 mutant backgrounds, complementation with the pVND7 promoter worked better than the pVND6 promoter (Figures 4 and 5). This difference must be due to the differences in the expression profiles of these promoters. Since both pVND6:IRX9 and pVND7:IRX9 lines show the same low xylan content in the walls, it is not because the pVND7 promoter is necessarily stronger than pVND6. The VND6 transcription factor gene is specifically expressed in metaxylem vessels, while VND7 has been shown to be expressed in both the protoxylem and metaxylem vessels [43, 49]. The broader expression pattern when expressing xylan biosynthetic genes under the VND7 promoter may account for the better growth complementation in these plants. Expression of xylan in the metaxylem only, with the pVND6:IRX7/IRX8/IRX9 constructs might not be sufficient to fully restore the irregular xylems of the irx mutants. This result contrasts with our recent study where the same pVND6 promoter construct was used to complement a mutant in lignin biosynthesis [50]. In that study, the pVND6:C4H construct fully complemented the irregular xylem phenotype of the c4h mutant. Such difference could be explained by the capability of the monolignols to diffuse in the cell wall prior to being polymerized into lignin in contrast to xylan polymers.

Irrespective of the promoter, complementation of irx7 worked better than irx9, which in turn worked better than irx8. The reason for this is not clear and it is difficult to speculate about it given the lack of knowledge about the biochemical function of the IRX7, IRX8 and IRX9 proteins. The three pVND7:IRX7 transformant lines all showed growth very similar to the wild type. The partial growth complementation seen for many of the other transformants was reflected in the still collapsed xylem vessels in these plants (Figures 6 and 7). The only transformants that showed the large open vessels characteristic for the wild type were the ones expressing the pVND7:IRX7 construct (Figure 7D1-3). In stem sections from the pVND7:IRX7 transformants, the fluorescence intensity of LM10 was similar to that of irx7 indicating that xylan levels were low, while the interfascicular fiber cell walls remained thin compared to the wild type. This result shows that it is possible to obtain plants that have reduced amounts of xylan in their walls, while still preserving the structural integrity of the xylem vessels.

Transformants expressing the pVND6/pVND7:IRX7/IRX8/IRX9 constructs showed decreased levels of xylan and lignin compared to wild type

The irx7, irx8 and irx9 mutants that were used as backgrounds for the transformations are xylan-deficient [33]. By expression of xylan biosynthetic genes specifically in the xylem vessels of these mutants, it was possible to rescue the strong growth phenotypes of the irx mutants, while all the transformed mutants still showed large decreases in xylose compared to the wild type, to levels resembling that of the respective irx mutant (Figure 8A) or to an intermediate level between the mutant and the wild type (Figure 8B). The three pVND7:IRX7 transformant lines with growth properties similar to wild type, had xylose contents that were 16-23% lower compared to the wild type.

Reductions in lignin has been proven to be important for decreasing the recalcitrance of biomass toward deconstruction, making the reductions in lignification observed here promising for increasing saccharification yields. The pVND6:IRX9 and pVND7:IRX9 transformants had reductions in lignin content to levels similar to that of the irx9 mutant (Figure 10A), while the transformants expressing the pVND6:IRX7 or pVND7:IRX7 construct had near wild type levels of lignin deposition (Figure 10B). That lignin deposition is affected in the complemented plants suggests that the degree of lignification of vascular tissues is dependent on xylan biosynthesis. There are several possible explanations for the decrease in lignin conferred by the loss of xylan. Since the transformants have an overall decrease in secondary wall development, the reduction in lignin may simply reflect that. However, the branches of GX polymers in Arabidopsis consist of GlcA and MeGlcA, and it is possible that the GlcA and MeGlcA substitutions have a function in interacting with lignin polymers by covalent attachment through esters [30]. Hence, there may be a more specific effect of the xylan reduction on lignin accumulation in the walls.

Transformants showed improved stem breaking strength

Wall integrity has been demonstrated to be compromised in the irx7, irx8 and irx9 mutants, causing a decrease in the breaking strength of the inflorescence stems [15, 35]. It is essential that plants bred or engineered for improved downstream processing do not have impaired growth or susceptibility e.g. to lodging. In general, the transformed irx mutants showed partial recovery of stem strength and several lines were as strong as the wild type. One of the transformant lines expressing the pVND7:IRX7 construct in the irx7 background was even 30% stronger than the wild type. Thus, it is possible to obtain plants that are not compromised in mechanical properties using the strategy described here.

The decrease in xylan and lignin content in the secondary walls in the transformants results in improved saccharification and a more optimal C6/C5 sugar ratio of hydrolyzates

The lower amounts of xylose and lignin observed in the secondary walls of the transformants were expected to yield higher saccharification efficiencies, as these two polymers are known to be the main contributors to cell wall recalcitrance [7]. We saw large increases in saccharification yields in all transformants compared to the wild type of up to 49% and a wild type like growth phenotype for the lines complemented with the pVND7:IRX7 construct. As inefficient enzymatic degradation of plant biomass is one of the major bottlenecks in achieving economically feasible biofuel production, the xylan engineering system we presented here is a great step toward tailored bioenergy crops that can alleviate the problem of biomass recalcitrance toward degradation. Furthermore, the hydrolyzates obtained by complete saccharification of the transformants have C6/C5 sugar ratios that are increased by up to 46% compared to the wild type.

The economic impact of improved feedstocks properties as reported in this paper is difficult to assess without pilot plant experiments. However, a very thorough techno-economical modeling of biomass to ethanol conversion allows good estimates to be made [55]. According to this model, a 20% decrease in xylose and 10% decrease in lignin content would result in about 10-15% decrease in minimum ethanol selling price, provided that plant growth would not be negatively impacted.

Engineering of bioenergy crops

The engineering approach described here was done in the model plant Arabidopsis. The future of tailored plants for biofuel production has been proposed to lie within fast growing plant species with high biomass yields. Fast growing C4 perennial grass species, such as Miscanthus (Miscanthus distachyon) and Switchgrass (Panicum virgatum) are promising as future bioenergy crop species, while hybrid poplar (e.g. Populus alba x tremula) show potential as a woody energy crop [6].

Several functional orthologs of the irx genes involved in xylan biosynthesis in Arabidopsis have been identified in hybrid poplar [56]. Here, GT47C[57] and GT8E/F[58] may function in the biosynthesis of the reducing end oligosaccharide of GX, as they are functional orthologs of IRX7/F8H and PARVUS, respectively, in Arabidopsis. GT8D is an ortholog of Arabidopsis IRX8 and has been shown to be important for maintaining the mechanical strength and xylan content in poplar, while GT43B has been shown to be a functional ortholog of Arabidopsis IRX9[59, 60]. The approach described in this paper depended on pre-existing mutants in irx genes, and such mutants may not be readily available in crop species. However, GT43B RNAi lines have been reported to have alterations in xylan content and xylan chain length that yield a reduction in recalcitrance to cellulose digestion [56]. These findings suggest that it will be possible to transfer our xylan engineering approach to poplar species in the near future by retransformation of plants where the native gene expression has been suppressed (e.g. by RNAi) with an RNAi-insensitive IRX allele driven by a vessel-specific promoter from poplar [61]. In grasses the situation is less clear, since the reducing end oligosaccharide of xylan has not been identified and it is unknown if there are functional orthologs of IRX7, IRX8 and PARVUS. However, grasses do have apparent orthologs of IRX9 and IRX9L and they could be targeted in a similar way through RNAi and transformation with a functional copy of IRX9 under control of a vessel-specific promoter. Orthologs of IRX10, which appears to be present in grasses [25], may be targeted in a similar way.

Transfer of the engineering approach to crop species, also requires vessel-specific promoters. Phylogenetic analysis suggests that VND6 and VND7 are highly conserved, and we expect that the Arabidopsis promoters will function in a wide range of species. If the expression level is too low to fully complement growth, extra copies of VND7 under control of its native promoter could be introduced. The findings, that Arabidopsis and poplar share many of the same biosynthetic networks [62, 63] sets the basis for introducing the transcription factor mediated xylan biosynthesis in poplar, the same way we have now demonstrated for Arabidopsis.


During this study, we have shown that it is possible to apply a xylan engineering approach by manipulating the spatial and temporal deposition of this abundant polymer specifically to the xylem vessels in mutant Arabidopsis plants deficient in GX biosynthesis. We obtained Arabidopsis plants that have up to a 23% reduction in xylose levels compared to wild type plants. These transformants exhibit wild type-like growth patterns and morphology and normal xylem vessels. Furthermore, these plants showed up to a 42% increase in saccharification yield after hot water pretreatment and 24 h of incubation with an enzyme mixture. The best results were obtained by transforming irx7 mutants with the pVND7:IRX7 construct. Several other plant lines in the irx9 and irx8 backgrounds yielded partial complementation of the irx phenotype thus showing promise of improvement in future experiments. The breaking-force tests show that the improvement in xylose-reduction and lignin content can be achieved without compromising mechanical strength of the plants.

The xylan engineering system developed in this study has the potential of being transferred to other biofuel crop species. Particularly poplar species have been shown to contain functional orthologs of the Arabidopsis IRX genes, and for the biosynthesis of cell wall polymers to be regulated by a transcriptional regulatory system similar to that in Arabidopsis.


Plant lines and growth conditions

All Arabidopsis wild type and mutant plant lines used are in the ecotype Columbia (Col-0) background. T-DNA insertion mutants (irx9-2, At2g37090, SALK_057033; irx7, At2g28110 SALK_120296; irx8-6, At5g54690, SALK_008642, [64]) were obtained from the Arabidopsis Biological Resource Center, Ohio State University, ( Wild type and T-DNA insertion mutant seeds were grown on soil at 22°C in a 16 h photoperiod after being stratified at 4°C for 4 days. Following transformation, seeds were harvested, sterilized and then grown on plates containing MS media (0.5x Murashige and Skoog salts, 7 g/l agar, 10 g/l sucrose) with 30 μg/ml hygromycin selection and stratified for 4 days at 4°C. Plates were then transferred to growth chambers at 22°C with 10 h photoperiod for 7–10 days. Positive transformant seedlings were transferred to soil.

Transformants in the irx9 background (except plants used for stem tests, expression analysis, and transgene screening, which were grown entirely with a 16 h photoperiod) were grown for 4 weeks at 22°C in 10 h photoperiod and then moved to 16 h photoperiod. Transformants in the irx7 and irx8 backgrounds were grown entirely with a 16 h photoperiod.

Vector constructs and Arabidopsis transformation

The native VND6 promoter containing a 2757 bp region upstream of the ATG codon was amplified from genomic DNA using the following primers, pVND6-F3-KpnI, cccgggtaccTCCTTTACGATGTTGTTATGGGTTA; pVND6-R3-SpeI, cccgactagtGTGTGCGAGA CTTTGGATTTGAT CTTTTTAATTTTA [50]. The native VND7 promoter containing a 2009 bp region upstream of the ATG codon was amplified from genomic DNA using gene specific primers pVND7NotI-5, CCCGGCGGCCGCTTCTGTAGTTCTTCTTCGGGTTTACAAATC; pVND7-NheI-3, CCCGGCTAGCATTATCCATCCACGATGATCCTATAAACGT. The PCR products were cloned into pBlunt (Invitrogen, Carlsbad, CA) to create pBlunt-pVND6 and pBlunt-pVND7 respectively. A Gateway cloning cassette was inserted between HindIII and AvrII restriction sites of the binary vector pCAMBIA 1390 (accession no. AF234307) to produce a pA6-GW vector. The promoter of VND6 was cut from pBlunt-pVND6 by KpnI and SpeI, and then inserted between KpnI and AvrII (SpeI compatible) restriction sites of the binary vector pA6-GW to produce the pA6-pVND6-GW vector. The promoter of VND7 was obtained by restriction digestion with KpnI and NheI from pBlunt-pVND7 and then inserted in the binary vector pA6-GW vector to produce the pA6-pVND7-GW vector.

The full-length coding regions of At2g28110 (IRX7), At5g54690 (IRX8) and At2g37090 (IRX9) were PCR amplified from Arabidopsis cDNA and cloned into pDONR/Zeo (Invitrogen) (for IRX7) and pCR8/GW/TOPO (Invitrogen) (for IRX8 and IRX9) by Gateway BP and Gateway TOPO reaction, respectively. LR reactions were set up using these entry vectors to clone the coding region into the Gateway compatible destination vectors pA6-pVND6-GW and pA6-pVND7-GW. After verification by sequencing, all constructs were transformed into Agrobacterium strain GV3101.

Homozygous irx9 mutants and heterozygous irx7 and irx8 plants were used for transformation with the floral dip method [65] for each of the above constructs, respectively. T1 seeds were sown on hygromycin plates and positive transformants were transferred to soil followed by subsequent verification of the genotype using PCR.

Screening of transformants for T-DNA insertions and transgenes

Identification of the positive transformants that were homozygous for the T-DNA insertions resulting in the irx9-2, irx7, and irx8-6 mutants were done as described by [33]. Primer sets of right- and left-border primers (RP+LP) specific for each T-DNA insertion were generated from the SIGnAL T-DNA Primer Design website ( as shown in Table 1.

Table 1 Plant lines and primers used for genotyping

To confirm the presence the transgene in the transformants, primer pairs were made for the respective pVND promoter and IRX gene combination and used in PCR reactions. Primer sequences used are shown in Table 2.

Table 2 Primers used to confirm presence and expression of the transgenes

Transcript analysis of transformants

RNA was isolated from stems using Qiagen RNeasy plant mini kit. First-strand cDNA synthesis was done using SuperScript II RT (Invitrogen). For the PCR steps, full-length gene-specific primer pairs were used. Primer sequences are shown in Table 2. (IRX7 forward 5’-ATGACAACACATAAACATAGAAGAAC-3’ and reverse 5’-CAAGAAAGAGTTTGACCTTCTAACA-3’; IRX9 forward 5’-ATGGGATCTCTAGAGAGATCA-3’ and reverse 5’-GGTGCTTAAACGTGTTCTTGTG-3’). ACTIN2 control was amplified using ACT2-fwd 5’-CTCAAA GACCAGCTCTTCCATC-3’ and ACT2-rev 5’-GCCTTTGATCTTGAGAGCTTAG-3’.

Monosaccharide composition analysis

Alcohol-insoluble residue (AIR) of inflorescence stems was prepared and destarched enzymatically as previously described [66]. For the irx7 and irx8 transformant lines, AIR was not destarched. All AIR samples were subsequently hydrolyzed with 2 M triflouroacetic acid (TFA) for 1 h at 120°C. For the irx9 transformant lines, completely dried senesced stem material was furthermore subjected to total sugar hydrolysis using the sulfuric acid method [67]. Samples were treated with 50 μl 72% w/w sulfuric acid and incubated for 1 h at 30°C while shaking. Samples were diluted with 715 μl of water and incubated at 120°C for 1 h. Sulfuric acid hydrolyzed samples were diluted 200-fold and the monosaccharide composition was determined by high-performance anion exchange chromatography (HPAEC) using a Dionex 3000 ion chromatograph as described [66].

Preparation of stem material for analysis by microscopy

The base of 6 week-old main inflorescence stems (2.5 cm distal from the rosette) were harvested and fixed overnight in fixative solution (4% paraformaldehyde in 50 mM piperazine-N,N-bis(2-ethanesulphonic acid) and 5 mM EGTA, pH 6.9) at 4°C as described in [68]. The stems were embedded in 7% agarose and cut into 60 μm thick sections using a Leica VT1000S vibratome and used for all subsequent microscopy analyses as described in [53].

Immunofluorescent labeling for light microscopy

Immunofluorescent labeling of transverse stem sections was done using the xylan-specific rat monoclonal antibody LM10 (Plant Probes) [52]. Sections were labeled as described in [68] with minor deviations. Sections were incubated with the primary antibody diluted 10-fold in a milk powder protein solution (5%, w/v) in phosphate buffered saline (PBS) for 1.5 h at room temperature. After extensive washes in PBS, sections were incubated in the dark with a secondary antibody (anti-rat/FITC) diluted 100-fold in PBS with 5% milk powder for 1.5 h at room temperature and washed again extensively with PBS. Pictures were taken using a Micropublisher Q-imaging camera (5.0 RTV) mounted on an epifluorescent microscope (Leica DM4000B) coupled with Metamorph software.

Force measurements of stem breaking force

Sections of main inflorescence stems from 100 to 150 mm above the rosette were taken from 7 week-old plants and the ultimate breaking force was measured using an in-house tensile testing instrument described previously [69].

Phloroglucinol-HCl staining of lignin

Fixed stem cross sections from each transformant line were treated one at a time with 2% phloroglucinol (Sigma, P3502) in a 2:1 ethanol/HCl solution [54]. The sections were analyzed on a Leica DM4000B microscope through the Bright-field filter.

Acetyl bromide assay for lignin quantification

Lignin quantification was determined by the acetyl bromide spectrophotometric method with some modifications [70, 71]. Acetyl bromide solution (600 μl of 25% v/v acetyl bromide in glacial acetic acid) was added to ~5 mg of AIR samples and incubated for 3 h at 50°C while shaking. Samples were cooled on ice to room temperature and centrifuged at 18407 g for 5 min. Subsequently, 100 μl of sample was transferred to a new tube. 400 μl of 2 M NaOH and 70 μl 0.5 M hydroxylamine hydrochloride was added followed by vortexing. 57 μl of each sample were transferred to a UV-transparent 96 well plate, filled up to 200 μl with glacial acetic acid and the samples analyzed in a plate reader at 280 nm.

Hot water pretreatment and saccharification

Cell wall pretreatment and saccharification was determined following a modified procedure from [54]. Dried, senesced stem material (5 mg fine powder) was pretreated with 200 μl of water and then incubated with shaking for 30 min at 30°C, followed by incubation for 1 h at 120°C. The samples were then allowed to cool to room temperature. For enzymatic saccharification, a mixture of 5 mg/ml tetracycline and Cellic CTec2 enzyme mix (Novozymes, Bagsværd, Denmark) in 0.1 M citrate buffer, pH 5.0 was added to the pretreated samples, followed by incubation at 50°C for 24 h at 900 rpm. Following addition of dinitrosalicylic acid reagent (1 g dinitrosalicylic acid and 30 g potassium sodium tartrate in 100 ml of 0.4 M NaOH) to the samples, aliquots were extracted and analyzed at the beginning of the experiment (T=0) and after 24 h (T=24). Samples were read on a plate reader at 540 nm. In addition, the released monosaccharides were analyzed by HPAEC as described above.