Open Access

Gene expression analysis of flax seed development

  • Prakash Venglat1,
  • Daoquan Xiang1,
  • Shuqing Qiu1,
  • Sandra L Stone1,
  • Chabane Tibiche2,
  • Dustin Cram1,
  • Michelle Alting-Mees1,
  • Jacek Nowak1,
  • Sylvie Cloutier3,
  • Michael Deyholos4,
  • Faouzi Bekkaoui1,
  • Andrew Sharpe1,
  • Edwin Wang2,
  • Gordon Rowland5,
  • Gopalan Selvaraj1 and
  • Raju Datla1Email author
Contributed equally
BMC Plant Biology201111:74

DOI: 10.1186/1471-2229-11-74

Received: 21 February 2011

Accepted: 29 April 2011

Published: 29 April 2011



Flax, Linum usitatissimum L., is an important crop whose seed oil and stem fiber have multiple industrial applications. Flax seeds are also well-known for their nutritional attributes, viz., omega-3 fatty acids in the oil and lignans and mucilage from the seed coat. In spite of the importance of this crop, there are few molecular resources that can be utilized toward improving seed traits. Here, we describe flax embryo and seed development and generation of comprehensive genomic resources for the flax seed.


We describe a large-scale generation and analysis of expressed sequences in various tissues. Collectively, the 13 libraries we have used provide a broad representation of genes active in developing embryos (globular, heart, torpedo, cotyledon and mature stages) seed coats (globular and torpedo stages) and endosperm (pooled globular to torpedo stages) and genes expressed in flowers, etiolated seedlings, leaves, and stem tissue. A total of 261,272 expressed sequence tags (EST) (GenBank accessions LIBEST_026995 to LIBEST_027011) were generated. These EST libraries included transcription factor genes that are typically expressed at low levels, indicating that the depth is adequate for in silico expression analysis. Assembly of the ESTs resulted in 30,640 unigenes and 82% of these could be identified on the basis of homology to known and hypothetical genes from other plants. When compared with fully sequenced plant genomes, the flax unigenes resembled poplar and castor bean more than grape, sorghum, rice or Arabidopsis. Nearly one-fifth of these (5,152) had no homologs in sequences reported for any organism, suggesting that this category represents genes that are likely unique to flax. Digital analyses revealed gene expression dynamics for the biosynthesis of a number of important seed constituents during seed development.


We have developed a foundational database of expressed sequences and collection of plasmid clones that comprise even low-expressed genes such as those encoding transcription factors. This has allowed us to delineate the spatio-temporal aspects of gene expression underlying the biosynthesis of a number of important seed constituents in flax. Flax belongs to a taxonomic group of diverse plants and the large sequence database will allow for evolutionary studies as well.


Flax (Linum usitatissimum L.) is a globally important agricultural crop grown both for its seed oil as well as its stem fiber. Flax seed is used as a food source and has many valuable nutritional qualities. The seed oil also has multiple industrial applications such as in the manufacture of linoleum and paints and in preserving wood and concrete. The fiber from flax stem is highly valued for use in textiles such as linen, specialty paper such as bank notes and in eco-friendly insulations [1]. Flax belongs to the family Linaceae and is one of about 200 species in the genus Linum [2]. It is a self-pollinating annual diploid plant with 30 chromosomes (2n = 30), and a relatively small genome size for a higher plant, estimated at ~700 Mbp [3, 4]. Although flax demonstrates typical dicotyledonous seed development, there are species-specific differences compared to, for instance, Arabidopsis thaliana seed development. However, very little is known about genes expressed during flax seed development. Advancing this knowledge and comparison of gene expression profiles and gene sequences would provide new insights into flax seed development.

Nutritionally, flax seed has multiple desirable attributes. It is rich in dietary fiber and has a high content of essential fatty acids, vitamins and minerals. The seeds are composed of ~45% oil, 30% dietary fiber and 25% protein. Around 73% of the fatty acids in flax seed are polyunsaturated. Approximately 50% of the total fatty acids consist of α-linolenic acid (ALA), a precursor for many essential fatty acids of human diet [5]. Flax seed is also a rich source of the lignan component secoisolariciresinol diglucoside (SDG). SDG is present in flax seeds at levels 75 - 800 times greater than any other crops or vegetables currently known [6, 7]. In addition to having anti-cancer properties, SDG also has antioxidant and phytoestrogen properties [8]. Flax seed contains about 400 g/kg total dietary fiber. This seed fiber is rich in pentosans and the hull fraction contains 2-7% mucilage [9]. The other major constituent of flax seeds are storage proteins that can range from 10-30% [10]. Globulins are the major storage proteins of flax seed, forming about 58-66% of the total seed protein [11, 12].

Improvement of flax varieties through breeding for various traits can be assisted by development of molecular markers and by understanding the genetic and biochemical bases of these characteristics [13, 14]. The goal of this research was to develop a comprehensive genomics-based dataset for flax in order to advance the understanding of flax embryo, endosperm and seed coat development. We report the construction of 13 cDNA libraries, each derived from specific flax seed tissue stages, as well as other vegetative tissues together with the generation of ESTs derived from these libraries and the related assembled unigenes. We mined the resulting database with the goal of revealing new insights into the gene expression in developing seeds in comparison to that of vegetative tissues and other plant species. We show the usefulness of this database as a tool to identify putative candidates that play critical roles in biochemically important pathways in the flax seed. Specifically we analyzed gene expression during embryogenesis as related to fatty acid, flavonoid, mucilage, and storage protein synthesis and transcription factors.

Results and Discussion

Seed development characteristics in flax

Limited information is available regarding flax seed development, despite its economic importance. Since the seed is an economically important output of this crop, in this study, we performed a detailed analysis of embryogenesis and flax seed development. The flax seed consists of three major tissues: the diploid embryo and triploid endosperm as products of double fertilization, and the maternal seed coat tissue. Soon after fertilization, the seed is translucent and the embryo sac is upright within the integuments (Figure 1A). The developing embryo is anchored at the micropylar end of the embryo sac. The thick, clear and fragile integuments of the fertilized ovule differentiate into the thin, dark and protective seed coat during seed development. Observation during the dissection process revealed that the endosperm initials, which formed at fertilization, undergo divisions to form a cellularized endosperm by the globular embryo stage (Figure 1B and Figure 2H). The endosperm progressively increases in size up to the torpedo stage, after which time it begins to degenerate, presumably to make space for the rapidly elongating cotyledons and to provide nutritional support to the developing embryo. By the late cotyledon stage the majority of endosperm cells have been consumed, leaving a thin layer of endosperm on the inner wall of the seed coat of the maturing seed.
Figure 1

Flax embryo development. (A) Cleared seed soon after fertilization. The embryo sac (arrow) encloses the embryo and endosperm and is anchored in the micropylar end (me) of the thick seed coat. (B-O) Scanning electron microscopy of developing flax embryo. (B) Dissected micropylar end of the seed showing endosperm cells (en) surrounding the developing globular embryo (em). (C) Globular embryo with suspensor anchored at the micropylar end. (D) Micropylar sleeve that remains after removal of the globular embryonic suspensor. (E) Globular embryo. (F) Heart embryo. The cotyledon primordia are indicated by "cp". (G) Early torpedo embryo. (H) Late torpedo embryos with pointed cotyledon tips. (I) Cotyledon stage embryo with rounded cotyledon tips. (J) Mature embryo with elongated cotyledons and a short embryonic axis. (K) Higher magnification of the cotyledon (co) and hypocotyl (hy) as indicated by the inset rectangle shown in (J). (L) The radicle tip showing the embryonic root apical meristem (ram). (M) The embryonic shoot apical meristem (sam) and leaf primordia (lp). Mature embryonic (N) cotyledon and (O) hypocotyl in cross-section to show cellular differentiation and storage deposits. Bar = 1 mm (J), 0.1 mm (A, B, G-I, K-O) and 10 μm (C-F).
Figure 2

Flax tissues used for cDNA library construction and EST analysis. (A) globular embryo; (B) heart embryo; (C) torpedo embryo; (D) cotyledon embryo; (E) mature embryo; (F) globular stage seed coat; (G) torpedo stage seed coat; (H) pooled endosperm from globular to torpedo stage seed; (I) etiolated seedlings; (J) stem; (K) stem peel "PS"; (L) leaves; and (M) mature flower.

The globular embryo (Figure 1C, 1E) has a short suspensor consisting of just four cells that is nestled into the micropylar sleeve (Figure 1D). As the embryo develops from the globular (Figure 1E) to heart (Figure 1F) and torpedo (Figure 1G) stages, the increase in embryo size is largely due to growth of the cotyledons. This is in contrast to the Arabidopsis embryo where the increase in size is due to an increase in both the cotyledons and the embryonic axis [15]. The embryonic axis consists of the hypocotyl and radicle initials that are formed at the heart stage and it eventually differentiates to form a short peg-like structure in the mature embryo. Whereas the tips of the cotyledon primordia are pointed in the late torpedo stages (Figure 1H) they become rounded at the top in the cotyledon stage (Figure 1I). The mature embryo (Figures 1J, 1K) is primarily composed of two large cotyledons, and a relatively short embryonic axis. The cotyledons play a dual role nutritionally during germination and early seedling growth. They hold much of the seed storage reserves and become photosynthetic after germination. The mature embryo contains dormant leaf primordia initials and shoot and root apical meristems that will become activated after imbibition and during the germination of the seed (Figures 1L, 1M). A cross-section of the cotyledon shows differentiation of the cortical cells into a layer of palisade cells and the compact mesophyll cells. The mesophyll cells of the cotyledon and the parenchyma cells of the hypocotyl are filled with storage deposits (Figure 1N, 1O) similar to those previously reported [16]. While flax seed development follows the general trends described for seeds of other model dicot species, there are some features that are different. For instance, unlike the Arabidopsis embryo, where the mature embryo is bent inside the anatropous seed, the flax embryo is positioned upright within the seed [15]. In the flax seed, the cotyledons take up the majority of the seed space with only a thin endosperm and seed coat left at maturity. This is in contrast to castor bean seeds where the endosperm is thick and the cotyledons nestled within the endosperm are thinner [17].

Sequencing 13 cDNA libraries provides insights into the flax transcriptome

The cDNA libraries constructed in this study provide a broad representation of seed development (8 libraries) as well as 5 libraries for vegetative tissues. The 8 seed libraries were all from the most widely cultivated Canadian linseed variety CDC Bethune and comprised globular embryo, heart embryo, torpedo embryo, cotyledon embryo, mature embryo, seed coat from the globular stage, seed coat from the torpedo stage and pooled endosperm (globular to torpedo stage) (Figure 2 A-H); four of the remaining five cDNA libraries were prepared from whole etiolated seedlings, stem, leaf, and flowers (Figure 2 I, J, L and 2M) of cv. CDC Bethune and the last library was for stem peels from cv. Norlin (Figure 2K).

The EST collection from single pass sequencing of the 3' end of the cDNA in plasmid clones had a median length of 613 nucleotides (nt). Each of these clones has been catalogued and stored at -80°C to allow for further studies. Full length cDNAs have also been identified for some clones by additional 5' end sequencing. Table 1 summarizes the distribution, quantity and quality of the ESTs obtained from the 13 libraries. After removal of vector sequences, rRNA sequences, sequences <80 nt, organelle sequences and masking for repeats, 261,272 sequences remained. The assembly of a final unigene set was done in two steps. First, ESTs from each library were assembled with EGassembler [18], resulting collectively in 27,168 contigs and 51,041 singletons. This collection of 78,209 contigs and singletons was reassembled with EGassembler. Thus a unigene set for each tissue source and a unified set of unigenes encompassing all the tissues were obtained. This second assembly process resulted in 15,784 contigs and 14,856 singletons, totaling 30,640 unigenes. The 30,640 unigenes identified here likely represents a major part of the flax seed transcriptome. Table 2 shows the distribution of the clusters, contigs, singletons and unigenes in the individual libraries. The length of the contigs varies from 102 to 3,027 nucleotides with a median length of 778 nt (data not shown). The sum of the lengths of the contigs plus singletons is 21.6 megabases, which represents 3% of the predicted 700Mb flax genome [3]. The EST distribution for each unigene among the 13 tissues and its predicted or putative Arabidopsis homologue is presented in Additional File 1. A queryable flax unigene database is available at and all the EST sequences are also deposited in GenBank (Table 3). Of the 30,640 unigenes, 23,418 (76.4%) were identified as having significant homology with Arabidopsis gene sequences. The Arabidopsis genome is ~157 Mbp [19] and has a transcriptome of ~27,000 genes [20] and our analysis hints that flax potentially has a larger transcriptome than Arabidopsis. While our libraries do not give complete coverage of the flax vegetative tissues, they can be used as minimum number to estimate the size of flax transcriptome.
Table 1

Distribution and analysis of flax ESTs in the 13 libraries

Tissue library

Number of ESTs sequenced

Number after cleaning

Number masked

% Trashed

Max length (nt)

Median length (nt)



































































































Minimum cut-off length for EST analysis was 80 nucleotides.

Table 2

Distribution of ESTs and unigenes (both contigs and singletons) in each library, and in the pooled data set (labeled Total)

Tissue library

Total ESTs in library

Number of clustered ESTs

Number of contigs

Number of singletons

Total number of unigenes per library

Number of contigs unique to library



































































































The last column states how many of the contigs were present in only one cDNA library, indicating potential tissue specific expression.

Table 3

GenBank accession numbers for the different flax EST libraries and their tissue source

GenBank Accession

Library Name

Tissue Source



Globular embryo



Heart embryo



Heart embryo



Torpedo embryo



Torpedo embryo



Cotyledon embryo



Mature embryo



Mature embryo



Globular seed coat



Torpedo seed coat



Endosperm pooled






Etiolated seedling









Stem peel




GO annotation and functional categorization

The unigene collection of 30,640 contigs and singletons was analyzed using the BLASTX algorithm against the UniProt-plants and TAIR databases. The unigenes that showed significant homology to known genes (E-value ≤ e-10) against UniProt-plants were selected for Gene Ontology (GO) annotation and further mapping of the GO terms to TAIR database which is manually and computationally curated on a ongoing basis [21]. The values generated for the different GO-categories were used to generate the classification based on molecular functions, biological processes and cellular components (Figure 3). Based on the BLAST analysis in TAIR, 23,418 unigenes showed significant homology to Arabidopsis genes and these are listed in a spreadsheet (Additional File 1; along with the distribution of ESTs for each unigene from the 13 tissue libraries. Our analysis suggests that the different GO-categories are well represented in our unigene dataset indicative of a broad coverage of expressed genes in the flax genome.
Figure 3

GO annotation of flax unigenes. TAIR annotation of flax unigenes indicates broad representation within each category. (A) Biological processes; (B) Molecular functions; (C) Cellular components. Numbers shown signify ESTs for each sub-category.

Hierarchical cluster analysis of flax tissue based EST collections

In order to compare the gene expression profile in different tissues, the entire set of 261,272 EST sequences was subjected to hierarchical cluster analysis using the software HCE3.5 [22] (see Methods). Amongst the parameters required for hierarchical cluster analysis, we selected the average linkage method and the Pearson correlation coefficient for the similarity/distance measure, a technique which has been widely used in microarray analysis [23]. The results are shown in Figure 4. The analysis shows that in general gene expression is most closely related in tissues that are developmentally related and connected. For example, globular (GE) and heart (HE) embryo stages are most closely related, followed closely by the torpedo stage (TE). The maturing embryos, viz., cotyledon (CE) and mature (ME) stages clustered together but were distantly placed from the early stage embryos. The two seed coat stages (GC and TC) also shared a relatively high degree of similarity to each other. Gene expression in the pooled endosperm tissue (EN) from early developing seed stages shared some similarity with early embryonic stages but was more distant from the seed coats and maturing embryos. It is interesting to note that the CE and ME stages cluster away from the early seed tissues (GE, HE, TE, GC, TC and EN) and to a lesser extent from other non-seed tissues viz., (ES, LE, FL, ST) which is indicative of the distinct seed maturation program that is occurring in the later stages of embryo development. As the stem peel (PS) did not contain all of the tissues normally present in whole stems (ST), and was enriched for the phloem and phloem fiber cells [24], the PS gene expression profile did not cluster with ST, and as expected was distantly placed from the rest of the vegetative tissues and seed tissues. Whole stems (ST) and etiolated seedlings (ES) showed a high degree of similarity, possibly due to their polysaccharide composition. Both whole stems and etiolated seedlings are likely to be particularly enriched in xylem tissues, the secondary walls of which produce polysaccharides different from those found in the pectin-enriched phloem fibers in (PS), seed coats (GC, TC), or the primary walls of developing embryos [25]. Taken together, this analysis showed three distinct patterns of relatedness of gene expression among the 13 tissues: early seed stages, the maturing embryo stages and the juvenile vegetative tissues (ES, ST and LF).
Figure 4

Hierarchical cluster analysis of flax EST libraries. Three gene expression clusters were identified, viz., early differentiating seed tissues, maturing embryos and juvenile vegetative tissues. The tree shows hierarchical clustering of the tissue-based libraries based on similarity/distance as measured by the Pearson correlation coefficient. Values close to 1 have high degree of similarity whereas lower values indicate the degree of distance between two libraries. Globular embryo (GE), heart embryo (HE), torpedo embryo (TE), cotyledon embryo (CE), mature embryo (ME), globular stage seed coat (GC), torpedo stage seed coat (TC), pooled endosperm (EN), etiolated seedlings (ES), stem (ST), stem peel (PS), leaves (LF), and mature flower (FL).

Nearly a fifth of the identified transcriptome is apparently unique to flax

To identify the degree of potential homology of the flax unigenes shared with other plant species, we performed BLASTX analysis against the proteomes representing the six fully sequenced and annotated genomes of Arabidopsis, Oryza sativa (rice), Sorghum bicolor (sorghum), Vitis vinifera (grape), Populus trichocarpa (poplar) and Ricinus communis (castor bean) (see Methods). In general, the deduced flax polypeptides are more similar to those of poplar and castor bean than to grape, Arabidopsis, sorghum or rice (Table 4). This is consistent with the taxonomic grouping of flax, poplar and castor bean within the order Malpighiales [26]. The order Malpighiales, which is a large diverse grouping of 42 families containing several economically important species, is hypothesized to have diverged within a relatively short time frame and the taxonomic relationship of families within this order is poorly resolved. However, genome sequencing of poplar [27], castor bean [28], cassava [29] and large EST libraries from other species within this order including flax (this study) will likely aid in molecular systematic studies to address broader phylogenetic relationships between these families. Whereas 66% of the unigenes (20,251) had hits in all six species, 16.8% (5,152) of the unigenes had no hits in any species, indicating that they may be flax specific genes.
Table 4

Flax unigenes are most similar to poplar and castor bean genes


Confidence level


x ≥ e-19


e-20≥ × ≥ e-49


e-50≥ × ≥ e-98


x ≤ e-99







Castor Bean

























Number of blast hits (BLASTX) of the 30,640 flax unigenes against six different plant genomes. Blast hit blocks indicate the confidence level with which the flax unigenes match other species' genes.

Key embryogenesis regulators are present in the EST collections

Transcription factors (TFs) are generally expressed at low levels and their presence in ESTs indicate the depth of the EST coverage. We analyzed the TFs present in all flax libraries. Among the TF families, three important motifs present in the TFs that regulate plant growth and development are the homeodomain (HD), MADS and the MYB domain [30]. TFs containing these domains are well represented in the 13 libraries and indicate good coverage of low expressed genes in the EST datasets (see Figure 5; Additional File 2). Overall, at least 783 transcription factors are present in the 30,640 flax unigenes.
Figure 5

Distribution of putative flax unigenes encoding MADS, homeodomain and MYB domain transcription factors. These transcription factor families are expected to have wide distribution and are found in majority of the flax EST libraries. EST distribution of flax unigenes used to compile this graph is listed in Additional File 2.

As one of the main objectives of this study was to gain a better understanding of what happens in the flax seed as it develops, we further analyzed the EST libraries for transcription factors with specific roles in embryo and seed development (Additional File 2). The establishment of the adaxial and abaxial polarity during cotyledon primordia differentiation at the heart stage of embryo development is specified by the HD-ZIPIII family, ASYMMETRIC LEAVES1 (AS1) (adaxial) and YABBY, KANADI families (abaxial) respectively [31]. ESTs corresponding to adaxial and abaxial polarity specifying TFs are expressed from globular stage onwards with maximum number of ESTs in the heart stage when the cotyledon primordia are specified (Figure 6; Additional File 2).
Figure 6

Putative flax unigenes representing organ polarity transcription factors. Organ polarity transcription factor ESTs are most abundant during cotyledon primordia differentiation of heart-stage embryos. Adaxial (HD-ZIPIII family and AS1) and abaxial (YABBY and KANADI families) gene expression establishes organ polarity. EST distribution of flax unigenes used to compile this graph is listed in Additional File 2.

LEAFY COTYLEDON (LEC) genes LEC1, LEC1-like (L1L), LEC2 and FUSCA3 (FUS3) are master regulators of embryogenesis that are primarily expressed throughout seed development, and ectopic expression of these TFs results in somatic embryogenesis or embryonic characteristics being overlaid on vegetative organs [3235]. ABI3 is expressed only during seed maturation and is a key regulator of seed maturation processes such as seed dormancy and storage reserve accumulation [36]. AGAMOUS-LIKE15 (AGL15), a MADS domain containing TF is primarily expressed during Arabidopsis seed development and its ectopic expression increases the competency of cells to respond to somatic embryogenesis induction conditions [37, 38]. In Arabidopsis, AGL15 is directly upregulated by LEC2 [39]. In addition, LEC2, FUS3 and ABI3 have all been demonstrated to be direct targets of AGL15 [40]. Examination of flax unigenes showed seed-specific enriched expression of L1L, LEC2, FUS3, ABI3 and AGL15 (Figure 7; Additional File 2). Only one EST with similarity to LEC2 was identified. The absence of LEC1 and the presence of the closely related L1L in seed tissues have also been observed for scarlett runner bean [33]. The identification of ESTs in seed-specific libraries that are pertinent to seed maturation program lends support to the quality of these libraries.
Figure 7

Putative flax unigenes encoding transcription factors that are known embryogenesis regulators. Tissue distribution of flax unigenes encoding ESTs with similarity to important regulators of embryogenesis are present in developing flax seed tissue libraries, and not in non-seed libraries. EST distribution of flax unigenes used to compile this graph is listed in Additional File 2.

Mining for biochemical pathway-specific ESTs that make flax seed nutritionally rich

The flax seed contains many nutritionally important compounds such as proteins, fatty acids, lignans, flavonoids and mucilage. To determine the usefulness of the EST resources generated in this study, we queried for genes involved in the synthesis of the above noted seed components. In order to identify potential candidate enzymes amongst many flax unigenes, the Additional Files 3 and 4 provide the first step to narrow down putative flax candidates by examining the timing and distribution of ESTs across different tissues.

Seed storage proteins

Much of the proteins in flax seeds are storage proteins that exist within protein storage vacuoles and these proteins constitute 23% of the whole flax seed [41]. Storage proteins in flax seed are made up of ~65% globulins and ~35% albumins [11]. Conlinin is a 2S albumin and cupin and cruciferin are 11S and 12S globulins, respectively. Our EST data correlates the expression of the genes coding for the storage proteins with the reported levels of proteins in flax seeds (Figure 8A; Additional File 3). Globulin encoding genes were expressed at much higher levels than those encoding the albumin and were observed in the later cotyledon (CE) and mature (ME) stages of embryo development. Interestingly, small numbers of ESTs for all the storage proteins were identified in young seed coats, primarily at the torpedo stage (Figure 8A; Additional File 3). This is in agreement with the observation that a conlinin gene promoter is active in early stages of seed coat development [42]. Pooled endosperm from the corresponding seed coat stages did not identify any storage protein ESTs. These observations suggest that the seed coat does have a role in storage protein synthesis. Given that the seed coat is a major part of the overall mass in developing seeds, the seed coat might be a transient source of protein for developing embryos.
Figure 8

EST distribution across tissue libraries of biosynthetic genes of important flax seed nutritional components. Fatty acid biosynthesis, oleosin oil body proteins and storage protein ESTs are highly represented in zygotic library compartments (A). Lignan, flavonoid and mucilage biosynthetic pathways are highly represented in maternal seed coat compartments (B). EST distribution of flax unigenes used to compile these graphs is listed in Additional File 3 and Additional File 4.

Fatty acids and oil body formation

Mature flax seeds consist of approximately 43% oil, mostly in the form of triacylglycerols (TAGs) within oil bodies located in the embryo [11]. In order to study the timing and source of lipid synthesis within the developing seeds, enzymes representing the four key steps of fatty acid synthesis were studied: acyl-chain elongation, termination, desaturation and TAG synthesis [43, 44] (Figure 8A, Figure 9; Additional File 3). Based on the preponderance of ESTs representing the 3-ketoacyl-acyl carrier protein synthases (KAS1, KAS2 and KAS3) in the various tissues, it appears that acyl chain elongation activity increases during the torpedo stage and that the embryo, endosperm and seed coat all contribute to this activity in the seed (Figure 9A). Although the number of ESTs representing termination of elongation by fatty acyl-ACP thioesterases (FATA and FATB) was lower than KAS ESTs, this activity also appears to peak during the torpedo stage (Figure 9B). Within the developing embryos, fatty acids are transferred onto a glycerol backbone to form triacylglycerols by the activity of diacylglycerol acyltransferase (DGAT). TAGs are stored in oil bodies, the outer membrane of which is a spherical phospholipid monolayer interspersed with the protein oleosin [44]. ESTs representing DGAT were found in quantities similar to the FATA and FATB ESTs, i.e. in very low quantities. The key difference is that this activity seems to peak later, during the cotyledon embryonic stage rather than the torpedo stage (Figure 9D). Also, while termination of elongation and release of free FAs appears to occur in both seed tissues as well as in some of the vegetative tissues, DGAT expression in vegetative tissues is too low to detect with the EST counts. Desaturation is the key step that results in the desirable omega-3 and omega-6 fatty acids [44]. This seems to occur later during seed development as the spike in the number of ESTs representing the Fatty Acid Desaturases (FAD) 2, 3, 5 and 8 occurs within the mature embryo (Figure 9C). One of the omega-3 fatty acids found in flax, alpha-linolenic acid (ALA, 18:3n-3), constitutes up to 55% of the total seed oil [41]. ALA is an essential fatty acid in human diet and it is converted to eicosapentaenoic acid (EPA) and docosahexaenoic acid (DHA) which are then incorporated into membrane phospholipids. Some fatty acids are used in plant membrane synthesis, wax formation and pigmentation. The repertoire of lipid synthesis ESTs found in stem, stem peel and flowers provide a basis to probe these processes in these tissues (Figures 8A and 9).
Figure 9

EST distribution of fatty acid biosynthetic genes during seed development and maturation across tissue libraries. (A) acyl chain elongation (Keto Acyl Synthases); (B) acyl chain termination (Fatty Acyl Thioesterases); (C) desaturation (Desaturases); (D) triacylglycerol (TAG) biosynthesis. EST distribution of flax unigenes used to compile these graphs is listed in Additional File 3.

Oleosins, proteins associated with oilbodies, are known to stabilize them by preventing the coalescence of the lipid particles during seed germination [45]. In our datasets, the expression of putative homologs of Arabidopsis Oleosin 1, 2 and 3 genes was observed in the embryo beginning at the torpedo stage (TE), with greater levels in mature stage (ME) (Figure 8A; Additional File 3). This also coincides with the expression in the CE and ME stages of the FAD desaturases that are involved in the formation of the omega-3 and omega-6 fatty acids. Oleosin gene expression has been shown to be regulated in part by ABI3 in Arabidopsis [46]. There is also a correlation of ABI3 with oleosin ESTs at the torpedo and mature embryo stages (Figure 7 and 8A; Additional File 2 and 3), indicating that the EST data is reflective of the underlying genetic and biochemical programs.


Flax is a rich source of secoisolariciresinol diglycoside (SDG). SDG is converted by intestinal bacteria to the so-called mammalian lignans enterodiol and enterolactone. SDG has phytoestrogen, antioxidant, and anticancer activities [8]. Lignans present in the seed coat of flax and are derived from coniferyl alcohol by the initial action of oxidases and dirigent proteins that yield pinoresinol [47]. Sequential reduction of pinoresinol by pinoresinol-lariciresinol reductase (PLR) results in the formation of SDG [48]. Analysis of our flax unigene collection identified several candidates corresponding to dirigent proteins and PLR that are predominantly expressed in the globular and torpedo stage seed coats (Figure 8B; Additional File 4). Dirigent proteins had a higher number of EST hits in globular stage seed coat which corresponds with its early role in the lignan biosynthetic pathway, whereas pinoresinol-lariciresinol reductase, which acts later in the pathway, is expressed in the seed coat at the torpedo stage.


Flavonoids constitute a major class of plant phenolics. Flax seeds are a rich source of flavonoids, which includes flavonols and anthocyanidins [49]. The flavonoid biosynthesis branch starts with the formation of chalcone, a reaction catalyzed by chalcone synthase (CHS), followed by the synthesis of flavanone by chalcone isomerase (CHI). Dihydroflavonol reductase (DFR) activity is the committing step for leucoanthocyanidin synthesis and proanthocyanidin, anthocyanidin and anthocyanin synthesis follows this step [50]. The key enzymes in the flavonoid synthesis pathway, viz., CHS, CHI and DFR are expressed during flax seed development especially in the seed coat tissues as shown by the number of ESTs (Figure 8B; Additional File 4). BANYULS (BAN) gene of Arabidopsis encodes an anthocyanidin reductase in the anthocyanidin branch that produces cis-3-flavan-3-ol which has known health benefits in humans [51]. ESTs representing BAN are present in the embryonic and seed coat tissues of flax indicating that flax seeds could be a likely source of cis-3-flavan-3-ols (Figure 8B; Additional File 4).

Mucilage synthesis and secretion

During flax seed development, the ovule integuments differentiate and form specialized cell types which include the seed coat epidermis that stores mucilaginous compounds. The chemical composition of flax seed mucilage has been investigated because of its benefits to human health. The pectin rhamnogalacturonan I (RG I) is the primary constituent of seed mucilage in Arabidopsis and several other species, whereas flax seed mucilage contains a mixture of neutral arabinoxylans (75%) and RG I (25%) [5254]. In the mature seed, the cells of the outer epidermal layer of the seed coat are transformed into mucilage secretory cells (MSCs) that release mucilage upon seed hydration. In Arabidopsis, MUCILAGE-MODIFIED4 (MUM4) gene encodes Rhamnose Synthase2, an enzyme that catalyzes the synthesis of RG I [55], whereas MUM2 encodes a beta-galactosidase that enables the hydration properties of the mucilage by modifying the RG I side chains [56]. Furthermore, AtBXL1 gene, which encodes a beta-xylosidase/alpha-arabinofuranosidase, is essential for the release of mucilage by degradation of the arabinan side chains in the mucilage and/or cell wall of the mucilage secretory cells [57]. Genes encoding rhamnose synthase and beta-xylosidase are represented in the GC and TC tissue specific ESTs indicating that the mucilage synthesis and secretion pathway observed in Arabidopsis is represented in flax and the expression of corresponding genes are enriched specifically in seed coat tissues (Figure 8B; Additional File 4). However, ESTs corresponding to the rhamnose synthase did not include the ortholog of Arabidopsis MUM4 gene, suggesting the possibility that there is some diversity of this mucilage synthesis pathway in flax. Galacturonosyltransferases that are involved in the polymerization of galacturonic acid [58] to form pectic RG I were also well represented in GC and TC tissue specific manner, indicative of their conserved roles in the synthesis of mucilage in the seed coat (Figure 8B; Additional File 4). Interestingly, ESTs corresponding to the putative homologs of the AtBXL2 gene, a member of the small gene family that includes AtBXL1 [57], were expressed at very high levels in the seed coat tissues suggesting their role in the quick and uniform release of mucilage from the flax seed coat upon imbibition (Figure 8B; Additional File 4). A putative flax ortholog of AtBXL1 is also one of the most abundant ESTs identified in a previous report of cDNAs from fiber-bearing flax tissues [59].


We have developed a comprehensive EST resource for flax representing developmental stages of specific seed tissues, some vegetative and reproductive tissues. These resources include publicly available EST sequences at GenBank (Table 3), a queryable flax unigene database ( and unigene distribution across libraries (Additional File 1). The datasets developed in this study enhance the genomic resource base for flax, an important crop. These resources can contribute to gene discovery and development of expanded molecular marker sets for breeding. Additionally, the unigene set developed in this study will contribute to the annotation and assembly of the whole flax genome sequence.

The recently published flax-specific microarray based on EST sequences obtained from a fiber focused study while the present manuscript was under preparation provides a complimentary genomic tool for flax gene expression analysis [60]. However, having the EST resources of the developing seed partitioned into embryo, endosperm, and seed coat compartments relative to vegetative tissues in our study allows further refinement into determining the involvement of genes in temporally and spatially specific metabolic pathways. Analysis of our datasets indicates good representation of biological processes related to seed development. 7,222 flax unigenes did not have homologs to the genes of the model species Arabidopsis and there were 5,152 unigenes that do not show any homology to plant species in UniProt. These 5,152 unigenes therefore likely represent flax-specific genes. Many of these unidentified genes were broadly distributed whereas some were specific to a single tissue. Further studies of these will provide new insights into flax-specific programs.

Materials and methods

Plant growth conditions and tissue collection

Breeder seed (F11) of Linum usitatissimum cv CDC Bethune was selfed for 7 generations (F18) as single plants in the Phytotron at the University of Saskatchewan. F19 seeds were germinated and grown in a growth chamber using a daily cycle consisting of 16 hours of light (23°C) and 8 hours of dark (16°C). Tissue samples were collected and frozen immediately in liquid nitrogen. The leaf, stem and flower samples were each collected from more than 10 individual plants. Dissection of 5,000 flax seeds was performed in order to isolate sufficient endosperm, embryonic, and seed coat tissues for creating the cDNA libraries. Five stages of embryos representing globular, heart, torpedo, cotyledon, and mature stages were isolated from developing seeds. Seed coat samples were collected from globular and torpedo embryo stages. Endosperm tissues were pooled from seeds containing globular to torpedo embryo stages. Etiolated seedlings were generated by incubating seeds on MS medium plates in the dark for four days and prior to harvesting, the seed coats were removed. The stem peel tissue consisting of epidermis, cortical tissues, phloem, developing fibers, and cambial tissue was prepared from stems of four week-old Linum usitatissimum L. cv Norlin germinated and grown as described previously [24].

RNA isolation and cDNA library construction

The stem peel library (PS) was constructed using the Superscript Plasmid System with Gateway Technology for cDNA Synthesis and Cloning (Invitrogen, Carlsbad, CA) [24]. cDNAs were directionally cloned in pCMV-SPORT6 (Invitrogen) and transformed in chemically competent DH5α-FT E. coli. For the remaining 12 libraries, total RNA was isolated using the RNeasy Plant Mini Kit (Qiagen, Cat. No. 74904). On-column DNase digestion was performed using the RNase-free DNase set (Qiagen, Cat. No. 79254). Approximately 2 μg of total RNA from the tissues was used to construct each cDNA library. These 12 libraries were constructed using the Creator SMART cDNA library construction kit (Clontech, Cat. N. 634903). The 8 libraries derived from seed tissues (globular, heart, torpedo, cotyledon and mature embryos, as well as endosperm and globular and torpedo stage seed coats) were prepared as per the manual instructions and are in the pDNR-lib vector (Clontech).

Two modifications to the manual were made during construction of the cDNA libraries for leaf, stem, flower and etiolated seedling. First, the cDNA size fractionation was performed on agarose gel instead of CHROMA SPIN-400 column supplied by the kit. The SfiI digested cDNAs were loaded into a 1% TAE agarose gel, and run for about 2 cm. The cDNA samples were excised from the agarose gel and purified using the QIAquick Gel Extraction kit (Qiagen, Cat. No. 28704). Second, a modified pBluescript II SK(+) vector was used. A ccdb gene, with SfiI sites at both ends, was inserted between the EcoRI and XhoI of pBluescript II SK(+). This modified vector was then digested with SfiI, agarose gel purified, and used for ligation with the SfiI digested cDNA samples. Ligations to construct the libraries were performed according to the Creator SMART manual.

EST sequencing and analysis

The libraries were spread onto the LB medium plates and cultured at 37°C overnight. Individual clones were picked into 96 or 384-plates manually or automatically by a Colony Picker (CP-7200, Norgren Systems). The ESTs were sequenced on the ABI 3730xl DNA Analyzer (Applied Biosystems) at the DNA sequencing facility of the National Research Council-Plant Biotechnology Institute (NRC-PBI, Saskatoon, SK, Canada). The HE, TE and ME libraries were sequenced in two batches (Table 3). A total of 274,278 sequences were obtained. The reader can refer to Table 1 for the tissue distribution. The assembling process of EGassembler was used. Details are given in the EGassembler tutorial [18] ( In the first step, the sequences were cleaned and ones with length of less than 100 bases were removed. The following steps consisted of masking the repeats, vector and organelle sequences. Masked nucleotides were removed and any resulting sequences less than 80 bases in length were also removed. The first clustering process was performed for each separate library. The resulting 78,209 sequences (27,168 contigs and 51,041 singletons) were then merged, and reassembled, resulting in 30,640 unigenes (15,784 contigs and 14,856 singletons). These unigenes were reallocated back into their respective individual libraries. All EST sequences and unigenes have been deposited at The clustering of the ESTs were performed using Hierarchical Clustering Explorer 3.5 sofware ( [22]. The number of EST reads for each unigene in each of the 13 different tissues was used as the input data for HCE3.5 software with parameters set for Pearson correlation coefficient for similarity/distance measure and average linkage method for hierarchical clustering.

BLASTX analysis of flax unigenes against the six plant genomes were performed using the proteomes from the respective species: Arabidopsis thaliana ''; Oryza sativa ''; Populus trichocarpa ''; Vitis vinifera '*'; Sorghum bicolor ''; and Ricinus communis from swissprot.



Fertilized ovules were cleared for 2 days in chloral hydrate solution (8:1:2 chloral hydrate - glycerol - water w/v/v) and viewed with a compound microscope (Leica DMR) using Nomarski optics.

Scanning Electron Microscopy

Samples were fixed in 3% glutaraldehyde, post-fixed in 1% osmium tetroxide and dehydrated in a graded acetone series as described [61]. Samples were mounted on aluminum stubs and coated with gold in an Edwards S150B sputter coater. Observations were made with a Phillips 505 scanning electron microscope at 30 kV and recorded on Fujifilm FP-100b professional film. Images were scanned and treated in Adobe Photoshop CS (Adobe Systems, San Jose, California) to improve the contrast and place scale bars.




This work was supported by National Research Council CEHH/NAPGEN and PPHS, Saskatchewan Agriculture Development Fund, Genome Canada and Genome Prairie TUFGEN programs. Rong Li provided the modified pBluescript II SK(+) vector. This is National Research Council of Canada publication number 50184.

Authors’ Affiliations

Plant Biotechnology Institute, NRC
Computational Chemistry and Bioinformatics Group, Biotechnology Research Institute, NRC
Cereal Research Centre, Agriculture and Agri-Food Canada
Department of Biological Sciences, University of Alberta
Crop Development Centre, University of Saskatchewan


  1. Vaisey-Genser M, Morris DH: History of cultivation and uses of flaxseed. Flax, The genus Linum. Edited by: Muir A, Westscott N. Amsterdam: Hardwood Academic Publishers, 2001, 1-21.Google Scholar
  2. Diederichsen A, Richards K: Cultivated flax and the genus Linum L.: Taxonomy and germplasm conservation. Flax, The genus Linum. Edited by: A. M, Westscott N. Amsterdam: Hardwood Academic Publishers, 2001, 22-54.Google Scholar
  3. Bennett MD, Leitch IJ: Plant DNA C-values database (release 3.0). 2004, []Google Scholar
  4. Cullis CA: DNA sequence organisation in the flax genome. Biochimica et Biophysica Acta (BBA) - Nucleic Acids and Protein Synthesis. 1981, 652: 1-15. 10.1016/0005-2787(81)90203-3.View ArticleGoogle Scholar
  5. Daun JK, DeClercq DR: Sixty years of Canadian flaxseed quality surveus at the Grain Research Laboratory. Proc of the Flax Institute of the United States. Fargo, ND.: Flax Institute of the United States, 1994, 192-200.Google Scholar
  6. Thompson LU, Rickard SE, Cheung F, Kenaschuk EO, Obermeyer WR: Variability in anticancer lignan levels in flaxseed. Nutrition and Cancer. 1997, 27: 26-30. 10.1080/01635589709514497.PubMedView ArticleGoogle Scholar
  7. Westcott ND, Muir AD: Variation in the concentration of the flaxseed lignan concentration with variety, location and year. Proc of the Flax Institute of the United States. Fargo, ND: Flax Institute of the United States, 1996, 56: 77-80.Google Scholar
  8. Touré A, Xueming X: Flaxseed Lignans: Source, Biosynthesis, Metabolism, Antioxidant Activity, Bio-Active Components, and Health Benefits. Comprehensive Reviews in Food Science and Food Safety. 2010, 9: 261-269. 10.1111/j.1541-4337.2009.00105.x.View ArticleGoogle Scholar
  9. Vaisey-Genser M, Morris DH: Flaxseed: Health, Nutrition and Functionality. 1997, Winnipeg, MB.: Flax Council of CanadaGoogle Scholar
  10. Oomah BD, Mazza G: Flaxseed proteins--a review. Food Chemistry. 1993, 48: 109-114. 10.1016/0308-8146(93)90043-F.View ArticleGoogle Scholar
  11. Westcott ND, Muir AD: Chemical studies on the constituents of Linum spp. Flax, the Genus Linum. 2001, Amsterdam: Hardwood Academic PublishersGoogle Scholar
  12. Chung MWY, Lei B, Li-Chan ECY: Isolation and structural characterization of the major protein fraction from NorMan flaxseed (Linum usitatissimum L.). Food Chemistry. 2005, 90: 271-279. 10.1016/j.foodchem.2003.07.038.View ArticleGoogle Scholar
  13. Cloutier S, Niu Z, Datla R, Duguid S: Development and analysis of EST-SSRs for flax (Linum usitatissimum L.). Theor Appl Genet. 2009, 119: 53-63. 10.1007/s00122-009-1016-3.PubMedView ArticleGoogle Scholar
  14. Cullis CA: Flax. Genome mapping and molecular breeding in plants - Oilseeds. Edited by: Kolle C. 2007, Berlin Heidelberg: Springer-Verlag, 2:Google Scholar
  15. Capron A, Chatfield S, Provart N, Berleth T: Embryogenesis: Pattern Formation from a Single Cell. The Arabidopsis Book. 2008, The American Society of Plant Biologists, 1-28.Google Scholar
  16. Ellis PR, Kendall CW, Ren Y, Parker C, Pacy JF, Waldron KW, Jenkins DJ: Role of cell walls in the bioaccessibility of lipids in almond seeds. The American Journal of Clinical Nutrition. 2004, 80: 604-613.PubMedGoogle Scholar
  17. Sachs J: Vorlesungen uber pflanzen-physiologie, Verlag Wilhem Engelmann, Leipzig. 1887, []Google Scholar
  18. Masoudi-Nejad A, Tonomura K, Kawashima S, Moriya Y, Suzuki M, Itoh M, Kanehisa M, Endo T, Goto S: EGassembler: online bioinformatics service for large-scale processing, clustering and assembling ESTs and genomic DNA fragments. Nucleic Acids Research. 2006, 34: W459-W462. 10.1093/nar/gkl066.PubMedPubMed CentralView ArticleGoogle Scholar
  19. Bennett MD, Leitch IJ, Price HJ, Johnston JS: Comparisons with Caenorhabditis (~100 Mb) and Drosophila (~175 Mb) Using Flow Cytometry Show Genome Size in Arabidopsis to be ~157 Mb and thus ~25% Larger than the Arabidopsis Genome Initiative Estimate of ~125 Mb. Annals of Botany. 2003, 91: 547-557. 10.1093/aob/mcg057.PubMedPubMed CentralView ArticleGoogle Scholar
  20. TAIR: 2009, []
  21. Berardini TZ, Mundodi S, Reiser L, Huala E, Garcia-Hernandez M, Zhang P, Mueller LA, Yoon J, Doyle A, Lander G, et al: Functional Annotation of the Arabidopsis Genome Using Controlled Vocabularies. Plant Physiol. 2004, 135: 745-755. 10.1104/pp.104.040071.PubMedPubMed CentralView ArticleGoogle Scholar
  22. Seo J, Gordish-Dressman H, Hoffman EP: An interactive power analysis tool for microarray hypothesis testing and generation. Bioinformatics. 2006, 22: 808-814. 10.1093/bioinformatics/btk052.PubMedView ArticleGoogle Scholar
  23. Thalamuthu A, Mukhopadhyay I, Zheng X, Tseng GC: Evaluation and comparison of gene clustering methods in microarray analysis. Bioinformatics. 2006, 22: 2405-2412. 10.1093/bioinformatics/btl406.PubMedView ArticleGoogle Scholar
  24. Roach MJ, Deyholos MK: Microarray analysis of flax (Linum usitatissimum L.) stems identifies transcripts enriched in fibre-bearing phloem tissues. Mol Genet Genomics. 2007, 278: 149-165. 10.1007/s00438-007-0241-1.PubMedView ArticleGoogle Scholar
  25. Gorshkova TA, Wyatt SE, Salnikov VV, Gibeaut DM, Ibragimov MR, Lozovaya VV, Carpita NC: Cell-Wall Polysaccharides of Developing Flax Plants. Plant Physiol. 1996, 110: 721-729.PubMedPubMed CentralGoogle Scholar
  26. Wurdack KJ, Davis CC: Malpighiales phylogenetics: Gaining ground on one of the most recalcitrant clades in the angiosperm tree of life. Am J Bot. 2009, 96: 1551-1570. 10.3732/ajb.0800207.PubMedView ArticleGoogle Scholar
  27. Tuskan GA, DiFazio S, Jansson S, Bohlmann J, Grigoriev I, Hellsten U, Putnam N, Ralph S, Rombauts S, Salamov A, et al: The Genome of Black Cottonwood, Populus trichocarpa (Torr. & Gray). Science. 2006, 313: 1596-1604. 10.1126/science.1128691.PubMedView ArticleGoogle Scholar
  28. Chan AP, Crabtree J, Zhao Q, Lorenzi H, Orvis J, Puiu D, Melake-Berhan A, Jones KM, Redman J, Chen G, et al: Draft genome sequence of the oilseed species Ricinus communis. Nat Biotech. 2010, 28: 951-956. 10.1038/nbt.1674.View ArticleGoogle Scholar
  29. Cassava Genome Project. 2010, []
  30. Riechmann JL, Ratcliffe OJ: A genomic perspective on plant transcription factors. Current Opinion in Plant Biology. 2000, 3: 423-434. 10.1016/S1369-5266(00)00107-2.PubMedView ArticleGoogle Scholar
  31. Bowman JL, Eshed Y, Baum SF: Establishment of polarity in angiosperm lateral organs. Trends in Genetics. 2002, 18: 134-141. 10.1016/S0168-9525(01)02601-4.PubMedView ArticleGoogle Scholar
  32. Lotan T, Ohto Ma, Yee KM, West MAL, Lo R, Kwong RW, Yamagishi K, Fischer RL, Goldberg RB, Harada JJ: Arabidopsis LEAFY COTYLEDON1 Is Sufficient to Induce Embryo Development in Vegetative Cells. Cell. 1998, 93: 1195-1205. 10.1016/S0092-8674(00)81463-4.PubMedView ArticleGoogle Scholar
  33. Kwong RW, Bui AQ, Lee H, Kwong LW, Fischer RL, Goldberg RB, Harada JJ: LEAFY COTYLEDON1-LIKE Defines a Class of Regulators Essential for Embryo Development. Plant Cell. 2003, 15: 5-18. 10.1105/tpc.006973.PubMedPubMed CentralView ArticleGoogle Scholar
  34. Stone SL, Kwong LW, Yee KM, Pelletier J, Lepiniec L, Fischer RL, Goldberg RB, Harada JJ: LEAFY COTYLEDON2 encodes a B3 domain transcription factor that induces embryo development. Proceedings of the National Academy of Sciences of the United States of America. 2001, 98: 11806-11811. 10.1073/pnas.201413498.PubMedPubMed CentralView ArticleGoogle Scholar
  35. Gazzarrini S, Tsuchiya Y, Lumba S, Okamoto M, McCourt P: The Transcription Factor FUSCA3 Controls Developmental Timing in Arabidopsis through the Hormones Gibberellin and Abscisic Acid. Developmental Cell. 2004, 7: 373-385. 10.1016/j.devcel.2004.06.017.PubMedView ArticleGoogle Scholar
  36. Parcy F, Valon C, Raynal M, Gaubier-Comella P, Delseny M, Giraudat J: Regulation of Gene Expression Programs during Arabidopsis Seed Development: Roles of the ABI3 Locus and of Endogenous Abscisic Acid. Plant Cell. 1994, 6: 1567-1582.PubMedPubMed CentralView ArticleGoogle Scholar
  37. Heck GR, Perry SE, Nichols KW, Fernandez DE: AGL15, a MADS Domain Protein Expressed in Developing Embryos. Plant Cell. 1995, 7: 1271-1282.PubMedPubMed CentralView ArticleGoogle Scholar
  38. Harding EW, Tang W, Nichols KW, Fernandez DE, Perry SE: Expression and Maintenance of Embryogenic Potential Is Enhanced through Constitutive Expression of AGAMOUS-Like 15. Plant Physiol. 2003, 133: 653-663. 10.1104/pp.103.023499.PubMedPubMed CentralView ArticleGoogle Scholar
  39. Braybrook SA, Stone SL, Park S, Bui AQ, Le BH, Fischer RL, Goldberg RB, Harada JJ: Genes directly regulated by LEAFY COTYLEDON2 provide insight into the control of embryo maturation and somatic embryogenesis. Proceedings of the National Academy of Sciences of the United States of America. 2006, 103: 3468-3473. 10.1073/pnas.0511331103.PubMedPubMed CentralView ArticleGoogle Scholar
  40. Zheng Y, Ren N, Wang H, Stromberg AJ, Perry SE: Global Identification of Targets of the Arabidopsis MADS Domain Protein AGAMOUS-Like15. Plant Cell. 2009, 21: 2563-2577. 10.1105/tpc.109.068890.PubMedPubMed CentralView ArticleGoogle Scholar
  41. DeClercq DR, Daun JK: Quality of Western Canadian Flaxseed. Canadian Grain Commission. 2002, []Google Scholar
  42. Truksa M, MacKenzie Samuel L, Qiu X: Molecular analysis of flax 2S storage protein conlinin and seed specific activity of its promoter. Plant Physiology and Biochemistry. 2003, 41: 141-147. 10.1016/S0981-9428(02)00022-0.View ArticleGoogle Scholar
  43. Ohlrogge JB, Jaworski JG: REGULATION OF FATTY ACID SYNTHESIS. Annual Review of Plant Physiology and Plant Molecular Biology. 1997, 48: 109-136. 10.1146/annurev.arplant.48.1.109.PubMedView ArticleGoogle Scholar
  44. Voelker T, Kinney AJ: VARIATIONS IN THE BIOSYNTHESIS OF SEED-STORAGE LIPIDS. Annual Review of Plant Physiology and Plant Molecular Biology. 2001, 52: 335-361. 10.1146/annurev.arplant.52.1.335.PubMedView ArticleGoogle Scholar
  45. Huang A: Oleosins and Oil Bodies in Seeds and Other Organs. Plant Physiol. 1996, 110: 1055-1061. 10.1104/pp.110.4.1055.PubMedPubMed CentralView ArticleGoogle Scholar
  46. Crowe AJ, Abenes M, Plant A, Moloney MM: The seed-specific transactivator, ABI3, induces oleosin gene expression. Plant Science. 2000, 151: 171-181. 10.1016/S0168-9452(99)00214-9.PubMedView ArticleGoogle Scholar
  47. Davin LB, Lewis NG: Dirigent Proteins and Dirigent Sites Explain the Mystery of Specificity of Radical Precursor Coupling in Lignan and Lignin Biosynthesis. Plant Physiol. 2000, 123: 453-462. 10.1104/pp.123.2.453.PubMedPubMed CentralView ArticleGoogle Scholar
  48. Ford JD, Huang KS, Wang HB, Davin LB, Lewis NG: Biosynthetic Pathway to the Cancer Chemopreventive Secoisolariciresinol Diglucoside-Hydroxymethyl Glutaryl Ester-Linked Lignan Oligomers in Flax (Linum usitatissimum) Seed†. Journal of Natural Products. 2001, 64: 1388-1397. 10.1021/np010367x.PubMedView ArticleGoogle Scholar
  49. Oomah BD, Giuseppe M, Kenaschuk EO: Flavonoid content of flaxseed. Influence of cultivar and environment. Euphytica. 1996, 90: 163-167. 10.1007/BF00023854.View ArticleGoogle Scholar
  50. Lepiniec L, Debeaujon I, Routaboul JM, Baudry A, Pourcel L, Nesi N, Caboche M: GENETICS AND BIOCHEMISTRY OF SEED FLAVONOIDS. Annual Review of Plant Biology. 2006, 57: 405-430. 10.1146/annurev.arplant.57.032905.105252.PubMedView ArticleGoogle Scholar
  51. Xie DY, Sharma SB, Paiva NL, Ferreira D, Dixon RA: Role of Anthocyanidin Reductase, Encoded by BANYULS in Plant Flavonoid Biosynthesis. Science. 2003, 299: 396-399. 10.1126/science.1078540.PubMedView ArticleGoogle Scholar
  52. Fedeniuk RW, Biliaderis CG: Composition and Physicochemical Properties of Linseed (Linum usitatissimum L.) Mucilage. Journal of Agricultural and Food Chemistry. 1994, 42: 240-247. 10.1021/jf00038a003.View ArticleGoogle Scholar
  53. Naran R, Chen G, Carpita NC: Novel Rhamnogalacturonan I and Arabinoxylan Polysaccharides of Flax Seed Mucilage. Plant Physiol. 2008, 148: 132-141. 10.1104/pp.108.123513.PubMedPubMed CentralView ArticleGoogle Scholar
  54. Cui W, Mazza G, Biliaderis CG: Chemical Structure, Molecular Size Distributions, and Rheological Properties of Flaxseed Gum. Journal of Agricultural and Food Chemistry. 1994, 42: 1891-1895. 10.1021/jf00045a012.View ArticleGoogle Scholar
  55. Western TL, Young DS, Dean GH, Tan WL, Samuels AL, Haughn GW: MUCILAGE-MODIFIED4 Encodes a Putative Pectin Biosynthetic Enzyme Developmentally Regulated by APETALA2, TRANSPARENT TESTA GLABRA1, and GLABRA2 in the Arabidopsis Seed Coat. Plant Physiol. 2004, 134: 296-306. 10.1104/pp.103.035519.PubMedPubMed CentralView ArticleGoogle Scholar
  56. Dean GH, Zheng H, Tewari J, Huang J, Young DS, Hwang YT, Western TL, Carpita NC, McCann MC, Mansfield SD, et al: The Arabidopsis MUM2 Gene Encodes a {beta}-Galactosidase Required for the Production of Seed Coat Mucilage with Correct Hydration Properties. Plant Cell. 2007, 19: 4007-4021. 10.1105/tpc.107.050609.PubMedPubMed CentralView ArticleGoogle Scholar
  57. Arsovski AA, Popma TM, Haughn GW, Carpita NC, McCann MC, Western TL: AtBXL1 Encodes a Bifunctional {beta}-D-Xylosidase/{alpha}-L-Arabinofuranosidase Required for Pectic Arabinan Modification in Arabidopsis Mucilage Secretory Cells. Plant Physiol. 2009, 150: 1219-1234. 10.1104/pp.109.138388.PubMedPubMed CentralView ArticleGoogle Scholar
  58. Harholt J, Suttangkakul A, Vibe Scheller H: Biosynthesis of Pectin. Plant Physiol. 2010, 153: 384-395. 10.1104/pp.110.156588.PubMedPubMed CentralView ArticleGoogle Scholar
  59. Day A, Addi M, Kim W, David H, Bert F, Mesnage P, Rolando C, Chabbert B, Neutelings G, Hawkins S: ESTs from the Fibre-Bearing Stem Tissues of Flax (Linum usitatissimum L.): Expression Analyses of Sequences Related to Cell Wall Development. Plant Biology. 2005, 7: 23-32. 10.1055/s-2004-830462.PubMedView ArticleGoogle Scholar
  60. Fenart S, Ndong YP, Duarte J, Riviere N, Wilmer J, van Wuytswinkel O, Lucau A, Cariou E, Neutelings G, Gutierrez L, et al: Development and validation of a flax (Linum usitatissimum L.) gene expression oligo microarray. BMC Genomics. 2010, 11: 592-10.1186/1471-2164-11-592.PubMedPubMed CentralView ArticleGoogle Scholar
  61. Venglat SP, Sawhney VK: Benzylaminopurine induces phenocopies of floral meristem and organ identity mutants in wild-type Arabidopsis plants. Planta. 1996, 198: 480-487. 10.1007/BF00620066.PubMedView ArticleGoogle Scholar


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