Browse Subject Areas

Click through the PLOS taxonomy to find articles in your field.

For more information about PLOS Subject Areas, click here.

  • Loading metrics

Analysis of Flavonoids and the Flavonoid Structural Genes in Brown Fiber of Upland Cotton

  • Hongjie Feng ,

    Contributed equally to this work with: Hongjie Feng, Xinhui Tian

    Affiliation The Key Laboratory of Oasis Eco-agriculture, Agriculture College of Shihezi University, Shihezi, China

  • Xinhui Tian ,

    Contributed equally to this work with: Hongjie Feng, Xinhui Tian

    Affiliation The Key Laboratory of Oasis Eco-agriculture, Agriculture College of Shihezi University, Shihezi, China

  • Yongchang Liu,

    Affiliation The Key Laboratory of Oasis Eco-agriculture, Agriculture College of Shihezi University, Shihezi, China

  • Yanjun Li,

    Affiliation The Key Laboratory of Oasis Eco-agriculture, Agriculture College of Shihezi University, Shihezi, China

  • Xinyu Zhang,

    Affiliation The Key Laboratory of Oasis Eco-agriculture, Agriculture College of Shihezi University, Shihezi, China

  • Brian Joseph Jones,

    Affiliation Faculty of Agriculture and Environment, University of Sydney, Sydney, Australia

  • Yuqiang Sun , (JS); (YS)

    Affiliation College of Life and Environmental Science, Hangzhou Normal University, Hangzhou, China

  • Jie Sun (JS); (YS)

    Affiliation The Key Laboratory of Oasis Eco-agriculture, Agriculture College of Shihezi University, Shihezi, China

Analysis of Flavonoids and the Flavonoid Structural Genes in Brown Fiber of Upland Cotton

  • Hongjie Feng, 
  • Xinhui Tian, 
  • Yongchang Liu, 
  • Yanjun Li, 
  • Xinyu Zhang, 
  • Brian Joseph Jones, 
  • Yuqiang Sun, 
  • Jie Sun



As a result of changing consumer preferences, cotton (Gossypium Hirsutum L.) from varieties with naturally colored fibers is becoming increasingly sought after in the textile industry. The molecular mechanisms leading to colored fiber development are still largely unknown, although it is expected that the color is derived from flavanoids.

Experimental Design

Firstly, four key genes of the flavonoid biosynthetic pathway in cotton (GhC4H, GhCHS, GhF3′H, and GhF3′5′H) were cloned and studied their expression profiles during the development of brown- and white cotton fibers by QRT-PCR. And then, the concentrations of four components of the flavonoid biosynthetic pathway, naringenin, quercetin, kaempferol and myricetin in brown- and white fibers were analyzed at different developmental stages by HPLC.


The predicted proteins of the four flavonoid structural genes corresponding to these genes exhibit strong sequence similarity to their counterparts in various plant species. Transcript levels for all four genes were considerably higher in developing brown fibers than in white fibers from a near isogenic line (NIL). The contents of four flavonoids (naringenin, quercetin, kaempferol and myricetin) were significantly higher in brown than in white fibers and corresponding to the biosynthetic gene expression levels.


Flavonoid structural gene expression and flavonoid metabolism are important in the development of pigmentation in brown cotton fibers.


Naturally colored cotton has innate color in the fiber. With a growing demand amongst consumers for environmentally benign products, naturally colored cotton, which can be used with little or no processing and dying steps, is becoming increasingly attractive to textile industries [1][3]. Unfortunately, however, only brown and green naturally colored varieties are currently available, restricting the development of naturally colored cotton textile market. It may be possible to increase the diversity of available naturally colored fibers using conventional breeding, however, this approach is limited by a lack of understanding of the process of cotton fiber color formation. In order to progress the integration of new natural colors into cotton, it is imperative that guidance is provided to molecular breeding programs. The fundamental requirement for this is an exploration and understanding of the molecular basis of pigment synthesis and deposition in cotton fibers.

Several genetic loci potentially involved in the process have been identified. A major loci with an incomplete dominant inheritance pattern for cotton fiber color formation has been identified [4][5]. It has also been reported that two or more loci are important for the inheritance of cotton fiber color [6]. Zhan et al. [5] showed that a pair of incomplete dominant loci controlled fiber color formation, and that there are several ‘minor loci’ that play additional roles. Shi et al. [7] concluded that green fiber was dominant to brown fiber, while brown fiber was dominant over white, and that there are genetic interactions between lint and fuzz color genes. Pure white fiber can be obtained by separating and extracting pigments from the colored cotton fiber, indicating that the pigment is independent and does not co-exist with the cellulose in the colored cotton fibers [8][9]. Extraction, washing and color reaction experiments indicated that pigments in brown fibers belong to the flavonoid group [10]. Whereas these studies have given us important clues, the precise molecular basis of pigment synthesis and deposition in cotton is still unknown and further studies are required before there is sufficient understanding to begin the process of introgressing novel color modifications into elite cotton varieties.

In plants, three major classes of flavonoids (anthocyanins, proanthocyanidins and flavonols) are synthesized via the branched flavonoid biosynthetic pathway [11][13]. These secondary metabolites contribute to the 'colorful' pigmentation of flowers, fruits, seeds and leaves and are involved in several physiological and biochemical processes in plants, including UV protection, insect attraction, herbivore defense and symbiosis [14][16]. Plants also utilize various colors conferred by anthocyanins to recruit pollinators and to attract animals for seed dispersal [12]. Flavonoid compounds are often produced in vegetative tissues under conditions of stress, such as high light intensity, cold, nutrient deficiency, pathogen attack, or senescence [17]. As a result of this wide ranging importance, the genetics and biochemistry of the flavonoid biosynthetic pathway has been intensively studied in several plant species [18][20]. These studies have indicated that flavonoid composition is remarkably varied, both among plant species and even in different tissues of an individual plant [11], [21][23]. The flavonoid biosynthetic pathway has been extensively described in multiple publications [11][12], [14], [16]. The generalized scheme of the pathway is shown in Fig. 1.

Figure 1. Schematic representation of the flavonoid biosynthetic pathway modified from [24][26].

C4H: Cinnamate-4-hydroxylase; 4CL: 4-Coumarate acyl-COA ligase; CHS: chalcone synthase; CHI: chalcone isomerase; F3′H: flavonoid-3′-hydroxylase; F3′5′H: flavonoid-3′5′-hydroxylase; FLS: flavonol synthase; DFR: dihydroflavonol reductase; ANS: Anthocyanidin synthase; 3GT: 3-O-glucosyltransferase.

To further explore the molecular basis of pigmentation in colored cotton fiber, we cloned four key genes of the flavonoid biosynthetic pathway in cotton (GhC4H, GhCHS, GhF3H, and GhF35H) and studied their expression profiles during the development of brown- and white cotton fibers (Gossypium hirsutum L.). We also analyzed the concentrations of four components of the flavonoid biosynthetic pathway, naringenin, quercetin, kaempferol and myricetin in brown- and white fibers at different developmental stages by high performance liquid chromatograph (HPLC).

Materials and Methods

Plant Material

Upland cotton (Xincai5, G. hirsutum L.) with brown fibers (Brown cotton) and its near-isogenic line (NIL) with white fibers (white cotton) were planted in an experimental field at Shihezi University (Xinjiang Autonomous Region, China) under normal agronomic management conditions. Ovules and fibers were excised carefully from developing flower buds or bolls on selected days post anthesis (every three days) and stored at –70 °C before use.

Extraction of Total RNA

Total RNA was extracted from fibers of 18 day post anthesis (DPA) brown- or white-fiber cotton fibers using a modified CTAB method [27] and were stored at −80°C. The quality of the total RNA was verified on 1% (w/v) ethidium bromide-stained agarose gel. The double-stranded cDNAs were synthesized from total RNA using an M-MLV reverse transcriptase (Invitrogen, SuperScript™II) by an anchored oligo-dT18 primer according to the manufacturer's instructions.

Cloning of flavonoid structural genes

Cotton flavonoid genes were isolated using a homologous sequence approach, based on conserved sequences of Arabidopsis Cinnamate-4-hydroxylase (C4H) and chalcone synthase (CHS), a Malus x domestica flavanone-3-hydroxylase (F3′H), a Petunia x hybrid flavonoid-3'5'-hydroxylase (F3′5′H) and a cDNA-AFLP differential fragment (between brown fiber and white fiber). These sequences were used as probes to match cotton ESTs in GenBank with the tBLASTn program ( The homologous ESTs were assembled into contigs using SeqMan program of DNAStar software (DNAStar, WI, USA), and the contigs were subjected to BLASTX analysis ( to scan for potential full-length ORFs. Subsequently, primers containing the putative ORFs were synthesized to amplify the cotton flavonoid structural genes, the cDNA derived from Xincai 5 brown fiber of 18 DPA was used as template (Table 1). The PCR products were cloned into T-cloning vector and sequenced. The predicted proteins were used to perform homology searches in GenBank using the BLASTP program ( To further characterize these cotton flavonoid structural genes, we performed multiple alignment and phylogenetic tree analyses using the predicted proteins and their homologs via CLUSTALW [28] in DNAStar (DNAStar, WI, USA), and the phylogenetic trees were viewed by TREEVIEW [29] program.

Table 1. The probe sequence, ESTs and Quantitative real-time PCR primers used in this study.

Expression analysis of the flavonoid structural genes

RNAs are extracted from roots (R), stems (S), leaves (L), petals (P) and fibers of 3, 6, 9, 12, 15, 18, 21, 24, 27 and 30 DPA of brown- and white-fiber cotton. The cDNAs were synthesized with a First-Strand cDNA Synthesis Kit (Promega) according to the manufacturer's instructions. The primers to specifically amplify PCR products of 200–300 bp from the four flavonoid structural genes were as listed Table 1. The Ubiquitin gene (UBI) was used as reference control, with the primers, 5′-CAG ATC TTC GTC AAA ACC CT-3′ and 5′-GAC TCC TTC TGG ATG TTG TA-3′ (GenBank Accession No. AI727463). Quantitative real-time PCR (QRT-PCR) were performed with the DNA Masterplus SYBR Green I Kit (Roche Applied Science) in a Mx3000p system (Agilent, USA). Each reaction (25 µL) contained 4 µM each primer, 2 µL cDNA(1∶100 diluted)and 10 µL PCR Buffer for Eva Green Master Mix. Thermal cycling conditions were pre-incubation 95 °C for 2 min, followed by 94 °C for 15 s, 56 °C for 20 s, and 72 °C for 20 s for 40 cycles. Each cDNA sample was run in duplicate. Relative expression ratios of target genes were calculated from the standard equation [30]. The expression assay was repeated three times and each assay was performed with three independent technical repeats. The means of the three biological experiments were calculated as the expression level of the genes.

Measurement of naringenin, quercetin, kaempferol and myricetin by HPLC

Naringenin, quercetin, kaempferol and myricetin from brown- and white-fibers (respectively 20 g) of 3, 6, 9, 12, 15, 18, 21, 24, 27 and 30 DPA were extracted into methanol/HCl (v∶v = 99∶1) for 12 h, then extracted using supersonic waves (40 KHZ, 250 W, 30 °C) for 30 mins. The extract was centrifuged (12, 000 g for 15 mins), concentrated (to 5 ml), and filtered (0.45 µm) [31][32].

The four components of flavonoid biosynthesis and metabolites were determined by reverse-phase HPLC using an HP1200 system (Agilent) with a Wakosil analytical column (250 mm×34.6 mm; 5 mm packing; SGE International). HPLC separation utilized a linear solvent gradient where Solvent A was acetonitrile and Solvent B was 1% acetic (v/v with water). The gradient conditions were: 0∼16 min, 30%∼49.8% A; 16∼18 min, 49.8%∼30% A; 18∼20 min, 30% A. The column was maintained at 30 °C and the flow rate was 0.4 mL/min. Measurements of the levels of the four secondary metabolites naringenin, quercetin, kaempferol and myricetin were determined based on commercial standards (Extra synthese), and the recovery rate was tested by internal standard method [33][34]. Each experiment was repeated 6 times.

Statistical analysis

Analysis of variance (ANOVA) and means were performed via the statistical software SPSS10.0.

Results and Discussion

Analysis of Genes Involved in Cotton Flavonoid Biosynthesis

Using a homologous sequence approach, the four flavonoid structural genes, designated: GhC4H (Genbank: EU921262), GhCHS1 (Genbank: EU921263), GhF3H (Genbank: GU062185) and GhF3′5′H (Genbank: GU062184) were cloned from upland cotton (Xincai5) fiber cDNAs. As shown in Table 2, the four genes encoded predicted proteins with high sequence similarity to corresponding proteins (including catalytically verified proteins) in GenBank.

Table 2. The proteins encoded by the flavonoid structural genes and the sequence similarity to their homologs.

CHS (chalcone synthase) is a key enzyme in the biosynthesis of anthocyanin [35]. GhCHS1 cloned from the brown cotton fibers was found to be a 1524 bp sequence containing an 1167 bp open read frame (ORF), encoding a predicted 389 amino acid polypeptide (Table 2). A multiple sequence alignment of GhCHS1 with homologous proteins revealed that it contained the conserved amino acids typical of chalcone synthase, including those at critical active sites (Cys164,His30,Ans336 and Phe215), five pocket substrate binding sites for 4-coumaroyl-CoA (Ser338,Thr197,Thr194,Glu192 and Ser133), and seven pocket sites (Thr132,Met137,Phe215,Ile254,Gly256,Phe265 and Pro375) for the cyclization reaction (Fig. 2). A phylogenetic tree constructed using 12 chalcone synthases from different species showed that the most closely related sequences to GhCHS1 were GhCHS and AmCHS from cotton and hollyhock (both Malvaceae), respectively. The most distantly related were OsCHS and ZmCHS, from the monocots rice and maize, respectively (Fig. 3 A).

Figure 2. Multiple alignment of deduced amino acid sequences of plant chalcone synthase.

Abbreviations of sequences RhCHS: Rosa hybrid cultivar 'Kardinal' (BAC66467); PcCHS: Pyrus communis (AAX16494); VvCHS:Vitis vinifera (BAB84111); AmCHS: Abelmoschus manihot(ACE60221); RsCHS: Rhododendron simsii (CAC88858).

Figure 3. Phylogenetic analyses of chalcone synthase and cytochrome P450 superfamily proteins from various species.

(A) Phylogenetic analyses of chalcone syntheses, (B) Phylogenetic analyses of cytochrome P450 superfamily proteins. VvCHS: Vitis vinifera (ABM67586), IpCHS: Ipomoeapurpurea (BAA20387), RhCHS: Rud-beckia hirta (ABN79673), ZmCHS: Zea mays (CAA42763), OsCHS: Oryza sativa (japonica cultivar-group) (BAA19186), AsCHS: Aquilaria sinensis (ABM73434), AtCHS; Arabidopsis thaliana (CAI30418), ThCHS: Torenia hybrid cultivar (BAB20074), AhCHS: Arachis hypogaea (AAO32821), AmCHS: Abelmoschus manihot (ACE60221); PhCHS: Petunia x hybrida (BAM17286); GhCHS: Gossypium hirsutum (ABS52573); PtC4H: Populus trichocarpa (ACC63873); HlC4H: Humulus lupulus (ACM69364); Ntc4h: Nicotiana tabacum (ABC69412); PhC4H: Petunia x hybrid (ADX33332); VvC4H: Vitis vinifera (XP_002266238); MdC4H: Malus x domestica (AAY87450); PaC3′H: Prunus avium (ADZ54783); VvC3′H: Vitis vinifera (XP_002284151); MdC3′H: Malus x domestica (ACR14867); ArC3′H: Arabidopsis lyrata subsp. Lyrata (XP_002871298); CsC3′H: Camellia sinensis (ACV74415); CiC3′H: Cichorium intybus (ACN65825); PtC3′5′H: Populus trichocarpa (XP_002314004); VvC3′5′H: Vitis vinifera (BAE47007); CsC3′5′H: Camellia sinensis (AAY23287); VwC3′5′H: Viola x wittrockiana (BAF93855); PiC3′5′H: Petunia integrifolia subsp. integrifolia (BAF34563); MtC3′5′H: Medicago truncatula (XP_003638760).

The three genes, GhC4H, GhF3′H and GhF3′5′H, belong to the cytochrome P450 superfamily, which includes other flavonoid synthetases (eg flavonol synthases, flavone synthases I, EC and enzymes involved in other pathways such as GA3-oxidases, GA2-oxidases, and aminocyclopropane carboxylic acid oxidases [36][37]. Multiple sequence alignment of the predicted GhC4H, GhF3H and GhF35H proteins with their homologous counterparts (Fig. 4) revealed that the proteins contained the domains typical of members of the cytochrome P450 superfamily, including the conserved active sites, the N-terminal domain CYP motif, ‘PPGP’, and the C-terminal domain Fe-binding site, and ‘FGAGRRICAG’ that forms a structure highly conserved in different species [38][39]. To study the relationship of GhC4H, GhF3′H, GhF3′5′H and other members of the family, a phylogenetic tree was constructed using 18 families of cytochrome P450s (Fig. 3 B). As shown in the phylogenetic tree, each protein family formed a unique clade, and GhC4H, GhF3H and GhF35H clustered in a clade that presumably corresponding to proteins of similar function.

Figure 4. Multiple alignment of deduced amino acid sequences of Cinnamate-4-hydroxylase (C4H), flavanone-3-hydroxylase (F3′H), flavonoid-3'5'-hydroxylase (F3′5′H) from the brown cotton fiber.

Expression profiles of cotton flavonoid structural genes

The expression of the four flavonoid structural genes, GhC4H, GhCHS1, GhF3H and GhF35H in roots (R), stems (S), leaves (L), petals (P) and fibers of 3, 6, 9, 12, 15, 18, 21, 24, 27 and 30 DPA brown and white fiber (Fig. 5) tissue was measured by QRT-PCR. All four genes were expressed, to a greater or lesser extent, in all tissues, but transcripts were considerably higher in cotton fibers. C4H is an important gene in the phenylalanine metabolic pathway, influencing many important traits through the synthesis of a large number of secondary metabolites, including lignins and flavonoids. Transcript levels for GhC4H were high in roots, stems, leaves and petals (Fig. 5 A). Transcript levels in the roots, stems, leaves and petals were lower for GhCHS1, GhF3H and GhF35H than for GhC4H (Fig. 5 B, C, D).

Figure 5. QRT-PCR analysis of four flavonoid structural genes in the brown and white cotton.

A: GhC4H1, B: GhCHS, C: GhF3H, D: GhF35H. In the horizontal axis, 1: roots; 2: hypocotyls; 3: leaves; 4: flowers, 5–14 represent 3, 6, 9, 12, 15, 18, 21, 24, 27, 30 DPA fiber cells, respectively.

During cotton fiber development, transcript levels for the four genes reached a maximum between 6–12 DPA, then declined rapidly. The GhC4H and GhCHS genes had high levels of transcripts in cotton fibers from the first measurement at 3 DPA, with the levels peaking at the 6 DPA. Transcript levels for GhF3H were high at 6 DPA, and peaked at 9 DPA. Transcript levels for F35H peaked at 9–12 DPA. Strikingly, transcript levels for all genes were substantially higher in brown fibers than in white fibers (Fig. 5 A, B, C, D). For example, while the peak of GhC4H transcript levels was measured at 6 DPA in both brown and white cotton fibers, the level in brown cotton fibers was 2.5 times higher than that measured in white cotton fiber (Fig. 5 A).

Together, these data show that the flavonoid structural genes are preferentially expressed in developing fibers and considerably higher levels of expression are associated with fiber from the brown cotton (Fig. 5). The data indicate that the flavonoid pathway and these genes are involved in the development of pigmentation in brown cotton fibers [40].

Changes of flavonoids content in developing cotton fibers

Using white cotton fiber as the control, the cumulative trend of naringenin, quercetin, kaempferol and myricetin concentrations in brown fibers were measured at different developmental stages by RP-HPLC. The recovery rates of naringenin (95.9%; RSD% = 1.85%), quercetin (99.2%; RSD% = 4.15%), kaempfero (96.3%; RSD% = 3.6%) and myricetin (98.7%; RSD% = 2.9%) were determined by comparing them with internal standards. As expected from the gene expression measurements, the concentration of the four flavonoids was significantly higher in brown fiber than in white fiber.

These four compounds are catalyzed in the flavonoid pathway to produce stable colorless precursors that are substrates for reactions that produce the pigment substances. Naringenin is the first stable intermediate product in the flavonoid synthesis pathway, and is the substrate for most flavonoids. During development of cotton fibers, the accumulation of naringenin was considerably higher in brown fibers than in white fibers. Naringenin reached to maximum concentration at 6 DPA in both brown and white fibers, but was significantly higher in brown than in white cotton fibers (0.22 µg/gFW in brown cotton fiber, 0.09 µg/gFW in white cotton fiber) (Fig. 6 A). Commensurate with flavonoid biosynthetic pathway gene expression, naringenin was undetectable after 21 DPA, indicating that it was completely converted to other flavonoids at this time. Quercetin concentrations increased dramatically from 15 to18 DPA (Fig. 6 B). Whereas kaempferol concentrations were low in brown cotton fibers (0.05 µg/gFW (Fig. 6 D), almost none of the compound could be detected in white fibers at any stage of development. The levels of myricetin in brown fibers were high from 6- 27 DPA, increased rapidly from 6 DPA and peaked (0.8 µg/gFW) at 12 DPA. By contrast myricetin levels remained very low in white fibers throughout development. (Fig. 6 C).

Figure 6. The contents of four flavonoids during the development of brown and white cotton fiber.

A: naringenin, B: quercetin, C: myricetin, D: kaempferol. The numbers in horizontal axis represent 3, 6, 9, 12, 15, 18, 21, 24, 27, 30 DPA fiber cells, respectively.

As both the flavonoid structural genes and the components of the flavonoid metabolic pathway were maintained at high levels in brown fibers compared to those observed in the white fiber NIL lines, our data suggest a significant role for the flavonoid pathway in brown cotton fiber development and a strong potential that compounds produced by the pathway are involved in the pigmentation of brown fibers. Meanwhile, the naringenin, quercetin, kaempferol and myricetin were the intermediate metabolites and the precursors for leucoanthocyanidins. We would like to track and identify the end product for the fiber color on the flavonoid pathway.

Relationship of gene expression and flavonoid accumulation in developing cotton fibers

During cotton fiber development, transcript levels for the four genes, GhC4H, GhCHS1, GhF3H and GhF35H, and the flavonoid levels were all higher in brown cotton fiber than they were in white cotton fibers from a NIL. The temporal pattern of transcript levels for all four genes was also consistent with timing of flavonoid accumulation in the cotton fibers. For example, GhC4H and GhCHS transcripts were high from the beginning of cotton fiber development, peaking at 6 DPA, then declining rapidly (Fig. 5 A and B). Naringenin accumulation coincided with this increase (Fig. 6 A). Furthermore, naringenin is the substrate for flavanone-3-hydroxylase (GhF3H), and transcript levels for this gene peaked between 6–9 DPA (Fig. 5 C), potentially explaining the peak of naringenin accumulation at 6 DPA.

In this paper, we analyzed four genes and four flavonoids in the flavonoid pathway in cotton fibers. The peak of transcript levels and the trends of flavonoloid accumulation were consistent and considerably higher in brown than in white cotton fibers, indicating their particular importance in the development of brown cotton fibers.


In summary, we compared the expression of genes involved in the flavonoid biosynthetic pathway in fibers from brown and white cotton (Gossypium hirsutum L.) using QRT-PCR, and analyzed trends in four flavonoids, naringenin, quercetin, kaempferol and myricetin at different stages of cotton fiber development by HPLC. The results showed that flavonoid structural gene expression and flavonoid accumulation were considerably higher in brown cotton fiber than in white cotton fiber, strongly suggesting that the flavonoid biosynthetic pathway contributes to the pigmentation of brown cotton fiber, This knowledge provides important information for unraveling cotton fiber pigmentation. We are confident that it is an important step in facilitating the development of new commercial cotton varieties with novel naturally colored fibres.

Author Contributions

Revised the paper: YCL BJJ. Conceived and designed the experiments: JS YQS. Performed the experiments: XHT HJF. Analyzed the data: XHT HJF. Contributed reagents/materials/analysis tools: JS YJL XYZ. Wrote the paper: HJF.


  1. 1. Vreeland JJM (1999) The revival of colored cotton. Scientific American 280: 112–119.
  2. 2. Qiu XM (2004) Research progress and prospects on naturally-colored cotton,Cotton Sciences. 16: 249–254.
  3. 3. Zhao XQ, Wang XD (2005) Composition Analysis of Pigment in Colored Cotton Fiber. Acta Agronomica Sinice 4: 456–462.
  4. 4. Kohel RJ (1985) Genetic analysis of fiber color variants in cotton. Crop Science 25: 793–797.
  5. 5. Zhan SH, Li ZP, Lin Y, Cai YP (2008) Quantitative analysis on the inherited characteristics of naturally colored brown cotton fiber color. Chinese Agricultural Science Bulletin 24: 146–148.
  6. 6. HlГlСимонгуrЯнl (1984) Genetic analysis of fiber color in upland cotton. Agron Abroad: Cotton 3: 172–191.
  7. 7. Shi YZ, Du XM, Liu GQ, Qiang AD, Zhou ZL, et al. (2002) Genetic Analysis of Naturally Colored Lint and Fuzz of Cotton. Cotton Sciences 14(4): 242–248.
  8. 8. Yatsu LY (1983) Ultrastructurel and chemical evidence that the cell wall of green fiber suberized. Plant Physiology 3: 521–524.
  9. 9. Ryser U, Meier H, Holloway PJ (1983) Identification and locailzation of suberin in the cell wall of green (Gossypium hirsutum L. Var. green lint). Protoplasma 117: 196–205.
  10. 10. Qiu XM, Zhou WL, Li MS, Ma YG (2002) Study on the genetics and production of fiber pigments and color deviation after wetting process of naturally colored cotton. Scientia Agricultura Sinica 35: 610–615.
  11. 11. Holton TA, Cornish EC (1995) Genetics and biochemistry of anthocyanin biosynthesis. Plant Cell 7: 1071–1083.
  12. 12. Winkel-Shirley B (2001) Flavonoid biosynthesis. A colorful model for genetics, biochemistry, cell biology, and biotechnology. Plant Physiology 126: 485–493.
  13. 13. Jaakola L, Maatta K, Pirttila AM, Törrönen R, Kärenlampi S, et al. (2002) Expression of genes involved in anthocyanin biosynthesis in relation to anthocyanin, proanthocyanidin, and flavonol levels during bilberry fruit development. Plant Physiology 30: 729–739.
  14. 14. Koes R, Verweij W, Quattrocchio F (2005) Flavonoids: a colorful model for theregulation and evolution of biochemical pathways. Trends Plant Science 10: 236–242.
  15. 15. Peters DJ, Constabel CP (2002) Molecular analysis of herbivore-induced condensed tannin synthesis: cloning and expression of dihydroflavonol reductase from trembling aspen (Populus tremuloides). Plant Journal 32: 701–712.
  16. 16. Gould KS, Lister C (2006) Flavonoid function in plants. In Flavonoids: Chemistry, biochemistry and applications. Edited by: Andersen M, Markham KR. Boca Raton, FL: CRC Press, 397–441.
  17. 17. Hernández I, Alegre L, Van Breusegem F, Munné-Bosch S (2009) How relevant are flavonoids as antioxidants in plants? Trends Plant Science 14: 125–132.
  18. 18. Korkina LG (2007) Phenylpropanoids as naturally occurring antioxidants: from plant defense to human health. Cell and Molecular Biology 53: 15–25.
  19. 19. Ververidis F, Trantas E, Douglas C, Vollmer G, Kretzschmar G, et al. (2007) Biotechnology of flavonoids and other phenylpropanoid-derived natural products. Part I: chemical diversity, impacts on plant biology and human health. Biotechnol Journal 2: 1214–1234.
  20. 20. Crozier A, Jaganath IB, Clifford MN (2009) Dietary phenolics: chemistry, bioavailability and effects on health. Natural Product Reports 26: 1001–1043.
  21. 21. Espley RV, Hellens RP, Putterill J, Stevenson DE, Kutty-Amma S, Allan AC (2007) Red colouration in apple fruit is due to the activity of the MYB transcription factor, MdMYB10. Plant Journal 49: 414–427.
  22. 22. Bogs J, Ebadi A, McDavid D, Robinson SP (2006) Identification of the flavonoid hydroxylases from grapevine and their regulation during fruit development. Plant Physiology 140: 279–291.
  23. 23. Castellarin SD, Di Gaspero G, Marconi R, Nonis A, Peterlunger E, et al. (2006) Colour variation in red grapevines (Vitis vinifera L.): genomic organisation, expression of flavonoid 3′-hydroxylase, flavonoid 3′,5′-hydroxylase genes and related metabolite profiling of red cyanidin-/blue delphinidin-based anthocyanins in berry skin. BMC Genomics doi:10.1186/1471-2164-7-12.
  24. 24. Boss PK, Davies C, Robinson SP (1996) Analysis of the expression of anthocyanin pathway genes in developing Vitis vinifera L. cv Shiraz grape berries and the implications for pathway regulation. Plant Physiology 111: 1059–1066.
  25. 25. Hummer W, Schreier P (2008) Analysis of proanthocyanidins. Molecular Nutrition & Food Research 52: 1381–1398.
  26. 26. Gutha LR, Casassa LF, Harbertson JF, Naidu RA (2010) Modulation of flavonoid biosynthetic pathway genes and anthocyanins due to virus infection in grapevine (Vitis vinifera L.) leaves. BMC Plant Biology doi:10.1186/1471-2229-10-187.
  27. 27. Luo M, Xiao YH, Hou L, Luo XY, Li DM, et al. (2003) Cloning and expression analysis of a LIM-domain protein gene from cotton (Gossypium hirsuturm L.). Journal of Genetics and Genomics 30: 175–182.
  28. 28. Thompson JD, Higgins DG, Gibson TJ (1994) CLUSTALW: improving the sensitivity of progressive multiple sequence alignment through sequence weighting, position-specific gap penalties and weight matrix choice. Nucleic Acids Research 22: 4673–4680.
  29. 29. Page RDM (1996) TREEVIEW: an application to display phylogenic trees on personal computers. Comput Application in the Biosciences 12: 357–358.
  30. 30. Bogs J, Downey MO, Harvey JS, Ashton AR, Tanner GJ, et al. (2005) Proanthocyanidin synthesis and expression of genes encoding leucoanthocy- anidin reductase and anthocyanidin reductase in developing grape berries and grapevine leaves. Plant Physiology 139: 652–663.
  31. 31. Hallt C, Ma Y, Buchbinder BU (1978) Messenger RNA for G1 protein of French bean seeds: Cell-free translation and product characterization. Proceedings of the National Academy of Sciences 75: 3196–320.
  32. 32. Constantine D Stalikas (2007) Extraction, separation, and detection methods for phenolic acids and flavonoids. Journal Separation Science 30: 3268–3295.
  33. 33. Chen HJ, Inbaraj BS, Chen BH (2011) Determination of Phenolic Acids and Flavonoids in Taraxacum formosanum Kitam by Liquid Chromatography- Tandem Mass Spectrometry Coupled with a Post-Column Derivatization Technique. International Journal of Molecular Sciences 13: 260–285.
  34. 34. Wang J, Zhao YM, Guo CY, Zhang SM, Liu CL, et al. (2012) Ultrasound-assisted extraction of total flavonoids from Inula helenium. Pharmacognosy Magazine 8: 166–170.
  35. 35. Lunkenbein S, Coine H, Devos CHR, Schaart JG, Boone MJ, et al. (2006) Molecular characterization of a stable antisense chalcone synthase phenotype in straw berry (Fragaria×ananassa). Journal of Agricultural and Food Chemistry 54: 2145–2153.
  36. 36. Hedden P, Phillips AL (2000) Gibberellin metabolism: new insights revealed by the genes. Trends Plant Science 5: 523–530.
  37. 37. Turnbull JJ, Nakajima J, Welford RWD, Yamazaki M, Saito K, et al. (2004) Mechanistic studies on three 2-oxoglutarate-dependent oxygenases of flavonoid biosynthesis: anthocyanidin synthase, flavonol synthase, and flavanone 3-hydroxylase. The Journal of Biological Chemistry 279: 206–1216.
  38. 38. Valegard K, Terwisscha AC, Scheltinga V, Lloyd MD, Hara T, et al. (1998) Structure of a cephalosporin synthase. Nature 394: 805–809.
  39. 39. Schoch GA, Attias R, Le Ret M, Dansette PM, Werck-Reichhart D (2003) Key substrate recognition residues in the active site of a plant cytochrome P450, CYP73A1. Homology guided site-directed mutagenesis. European Journal of Biochemistry 270: 3684–3695.
  40. 40. Xiao YH, Zhang ZS, Yin MH, Luo M, Li XB, et al. (2007) Cotton flavonoid structural genes related to the pigmentation in brown fibers. Biochemical and Biophysical Research Communications 358: 73–78.