Transgenic and Genome Editing Approaches for Modifying Plant Oils

  • Laura L. Wayne
  • Daniel J. Gachotte
  • Terence A. Walsh
Part of the Methods in Molecular Biology book series (MIMB, volume 1864)


Vegetable oils are important for human and animal nutrition and as renewable resources for chemical feedstocks. We provide an overview of transgenic and genome editing approaches for modifying plant oils, describing useful model and crop systems and different strategies for transgenic modifications. We also describe new genome editing approaches that are beginning to be applied to oilseed plants and crops. These approaches are illustrated with examples for modifying the nutritional quality of vegetable oils by altering fatty acid desaturation, producing non-native fatty acids in oilseeds, and enhancing the overall accumulation of oil in seeds and leaves.

Key words

Lipid biosynthesis Metabolic engineering Fatty acid Polyunsaturated fatty acids (PUFAs) Healthy oils Industrial oils CRISPR Genome editing Fatty acid desaturase Acyl transferase 


  1. 1.
    Wells R et al (2014) The control of seed oil polyunsaturate content in the polyploid crop species Brassica napus. Mol Breed 33:349–362PubMedCrossRefGoogle Scholar
  2. 2.
    Colbert T et al (2001) High-throughput screening for induced point mutations. Plant Physiol 126(2):480–484PubMedPubMedCentralCrossRefGoogle Scholar
  3. 3.
    Stephenson P et al (2010) A rich TILLING resource for studying gene function in Brassica rapa. BMC Plant Biol 10:62PubMedPubMedCentralCrossRefGoogle Scholar
  4. 4.
    Pollack A (2013) In a Bean, a Boon to Biotech, in New York TimesGoogle Scholar
  5. 5.
    Napier JA et al (2014) Understanding and manipulating plant lipid composition: metabolic engineering leads the way. Curr Opin Plant Biol 19:68–75PubMedPubMedCentralCrossRefGoogle Scholar
  6. 6.
    Voytas DF (2013) Plant genome engineering with sequence-specific nucleases. Annu Rev Plant Biol 64(1):327–350PubMedCrossRefPubMedCentralGoogle Scholar
  7. 7.
    Bates PD, Stymne S, Ohlrogge J (2013) Biochemical pathways in seed oil synthesis. Curr Opin Plant Biol 16(3):358–364PubMedCrossRefGoogle Scholar
  8. 8.
    Li-Beisson Y et al (2010) Acyl-lipid metabolism. Arabidopsis Book 8:e0133PubMedPubMedCentralCrossRefGoogle Scholar
  9. 9.
    Clough SJ, Bent AF (1998) Floral dip: a simplified method for agrobacterium-mediated transformation of Arabidopsis thaliana. Plant J 16(6):735–743PubMedPubMedCentralCrossRefGoogle Scholar
  10. 10.
    Browse J, McCourt P, Somerville CR (1985) A mutant of Arabidopsis lacking a chloroplast-specific lipid. Science 227(4688):763–765PubMedCrossRefGoogle Scholar
  11. 11.
    Gachotte D, Meens R, Benveniste P (1995) An arabidopsis mutant deficient in sterol biosynthesis - heterologous complementation by ERG-3 encoding a delta(7)-sterol-C-5-desaturase from yeast. Plant J 8(3):407–416PubMedCrossRefGoogle Scholar
  12. 12.
    Katavic V et al (1995) Alteration of seed fatty-acid composition by an ethyl methanesulfonate-induced mutation in arabidopsis-thaliana affecting diacylglycerol acyltransferase activity. Plant Physiol 108(1):399–409PubMedPubMedCentralCrossRefGoogle Scholar
  13. 13.
    Kumar R et al (2006) A mutation in Arabidopsis cytochrome b5 reductase identified by high-throughput screening differentially affects hydroxylation and desaturation. Plant J 48(6):920–932PubMedCrossRefGoogle Scholar
  14. 14.
    Miquel M, Browse J (1998) Arabidopsis lipids: a fat chance. Plant Physiol Biochem 36(1–2):187–197CrossRefGoogle Scholar
  15. 15.
    Somerville C, Browse J (1991) Plant lipids: metabolism, mutants, and membranes. Science 252(5002):80PubMedCrossRefGoogle Scholar
  16. 16.
    Beisson F et al (2003) Arabidopsis genes involved in acyl lipid metabolism. A 2003 census of the candidates, a study of the distribution of expressed sequence tags in organs, and a web-based database. Plant Physiol 132(2):681–697PubMedPubMedCentralCrossRefGoogle Scholar
  17. 17.
    Burgos A et al (2011) Analysis of short-term changes in the Arabidopsis thaliana glycerolipidome in response to temperature and light. Plant J 66(4):656–668PubMedCrossRefGoogle Scholar
  18. 18.
    Li Y et al (2006) Oil content of Arabidopsis seeds: the influence of seed anatomy, light and plant-to-plant variation. Phytochemistry 67(9):904–915PubMedCrossRefGoogle Scholar
  19. 19.
    Li Q et al (2015) Understanding the biochemical basis of temperature-induced lipid pathway adjustments in plants. Plant Cell 27(1):86–103PubMedPubMedCentralCrossRefGoogle Scholar
  20. 20.
    Stuitje AR et al (2003) Seed-expressed fluorescent proteins as versatile tools for easy (co)transformation and high-throughput functional genomics in Arabidopsis. Plant Biotechnol J 1(4):301–309PubMedCrossRefGoogle Scholar
  21. 21.
    Adhikari ND, Bates PD, Browse J (2016) WRINKLED1 rescues feedback inhibition of fatty acid synthesis in hydroxylase-expressing seeds. Plant Physiol 171(1):179–191PubMedPubMedCentralCrossRefGoogle Scholar
  22. 22.
    Llave C, Kasschau KD, Carrington JC (2000) Virus-encoded suppressor of posttranscriptional gene silencing targets a maintenance step in the silencing pathway. Proc Natl Acad Sci 97(24):13401–13406PubMedCrossRefGoogle Scholar
  23. 23.
    Wood CC et al (2009) A leaf-based assay using interchangeable design principles to rapidly assemble multistep recombinant pathways. Plant Biotechnol J 7(9):914–924PubMedCrossRefGoogle Scholar
  24. 24.
    Cernac A, Benning C (2004) WRINKLED1 encodes an AP2/EREB domain protein involved in the control of storage compound biosynthesis in Arabidopsis. Plant J 40(4):575–585PubMedCrossRefGoogle Scholar
  25. 25.
    Stone SL et al (2001) LEAFY COTYLEDON2 encodes a B3 domain transcription factor that induces embryo development. Proc Natl Acad Sci U S A 98(20):11806–11811PubMedPubMedCentralCrossRefGoogle Scholar
  26. 26.
    Vanhercke T et al (2013) Synergistic effect of WRI1 and DGAT1 coexpression on triacylglycerol biosynthesis in plants. FEBS Lett 587(4):364–369PubMedCrossRefGoogle Scholar
  27. 27.
    Liu F et al (2015) Enhanced seed oil content by overexpressing genes related to triacylglyceride synthesis. Gene 557(2):163–171PubMedCrossRefGoogle Scholar
  28. 28.
    Kinney AJ (1996) Development of genetically engineered soybean oils for food applications. J Food Lipids 3(4):273–292CrossRefGoogle Scholar
  29. 29.
    Cahoon EB et al (1999) Biosynthetic origin of conjugated double bonds: production of fatty acid components of high-value drying oils in transgenic soybean embryos. Proc Natl Acad Sci U S A 96(22):12935–12940PubMedPubMedCentralCrossRefGoogle Scholar
  30. 30.
    Cahoon EB et al (2000) Production of fatty acid components of meadowfoam oil in somatic soybean embryos. Plant Physiol 124(1):243–251PubMedPubMedCentralCrossRefGoogle Scholar
  31. 31.
    Li S et al (2017) Optimization of agrobacterium-mediated transformation in soybean. Front Plant Sci 8:246PubMedPubMedCentralGoogle Scholar
  32. 32.
    Govindarajulu M et al (2008) Evaluation of constitutive viral promoters in transgenic soybean roots and nodules. Mol Plant-Microbe Interact 21(8):1027–1035PubMedCrossRefGoogle Scholar
  33. 33.
    Curtin SJ et al (2011) Targeted mutagenesis of duplicated genes in soybean with zinc-finger nucleases. Plant Physiol 156(2):466–473PubMedPubMedCentralCrossRefGoogle Scholar
  34. 34.
    Haun W et al (2014) Improved soybean oil quality by targeted mutagenesis of the fatty acid desaturase 2 gene family. Plant Biotechnol J 12(7):934–940PubMedCrossRefGoogle Scholar
  35. 35.
    Moloney MM, Walker JM, Sharma KK (1989) High efficiency transformation ofBrassica napus usingAgrobacterium vectors. Plant Cell Rep 8(4):238–242PubMedCrossRefPubMedCentralGoogle Scholar
  36. 36.
    Nath UK et al (2009) Increasing erucic acid content through combination of endogenous low polyunsaturated fatty acids alleles with Ld-LPAAT + Bn-fae1 transgenes in rapeseed (Brassica napus L.). Theor Appl Genet 118(4):765–773PubMedCrossRefGoogle Scholar
  37. 37.
    De Block M, De Brouwer D, Tenning P (1989) Transformation of Brassica napus and Brassica oleracea using agrobacterium tumefaciens and the expression of the bar and neo genes in the transgenic plants. Plant Physiol 91(2):694–701PubMedPubMedCentralCrossRefGoogle Scholar
  38. 38.
    Guo XJ et al (2017) Identification and characterization of an efficient acyl-CoA: diacylglycerol acyltransferase 1 (DGAT1) gene from the microalga Chlorella ellipsoidea. BMC Plant Biol 17:16CrossRefGoogle Scholar
  39. 39.
    Shi JH et al (2017) Depressed expression of FAE1 and FAD2 genes modifies fatty acid profiles and storage compounds accumulation in Brassica napus seeds. Plant Sci 263:177–182PubMedCrossRefGoogle Scholar
  40. 40.
    Verma SS, Chinnusamy V, Bansa KC (2008) A simplified floral dip method for transformation of Brassica napus and B. carinata. J Plant Biochem Biotechnol 17(2):197–200CrossRefGoogle Scholar
  41. 41.
    Maheshwari P, Selvaraj G, Kovalchuk I (2011) Optimization of Brassica napus (canola) explant regeneration for genetic transformation. New Biotechnol 29(1):144–155CrossRefGoogle Scholar
  42. 42.
    Lu C, Kang J (2008) Generation of transgenic plants of a potential oilseed crop Camelina sativa by agrobacterium-mediated transformation. Plant Cell Rep 27(2):273–278PubMedCrossRefGoogle Scholar
  43. 43.
    Bansal S, Durrett TP (2016) Camelina sativa: an ideal platform for the metabolic engineering and field production of industrial lipids. Biochimie 120:9–16PubMedCrossRefGoogle Scholar
  44. 44.
    Haslam RP et al (2016) Synthetic redesign of plant lipid metabolism. Plant J 87(1):76–86PubMedPubMedCentralCrossRefGoogle Scholar
  45. 45.
    Rani T et al (2013) Genetic transformation in oilseed brassicas - a review. Indian J Agr Sci 83(4):367–373Google Scholar
  46. 46.
    Qi WC et al (2014) Regeneration and transformation of Crambe abyssinica. BMC Plant Biol 14:12CrossRefGoogle Scholar
  47. 47.
    Chen GQ (2011) Effective reduction of chimeric tissue in transgenics for the stable genetic transformation of lesquerella fendleri. Hortscience 46(1):86–90Google Scholar
  48. 48.
    Chen GQ et al (2016) Expression of castor LPAT2 enhances ricinoleic acid content at the sn-2 position of triacylglycerols in lesquerella seed. Int J Mol Sci 17(4):507PubMedPubMedCentralCrossRefGoogle Scholar
  49. 49.
    Parveez GKA et al (2015) Biotechnology of oil palm: strategies towards manipulation of lipid content and composition. Plant Cell Rep 34(4):533–543PubMedCrossRefGoogle Scholar
  50. 50.
    Izawati AM, Parveez GK, Masani MY (2012) Transformation of oil palm using agrobacterium tumefaciens. Methods Mol Biol 847:177–188PubMedCrossRefGoogle Scholar
  51. 51.
    McKeon TA et al (2014) Toxin content of commercial castor cultivars. J Am Oil Chem Soc 91(9):1515–1519CrossRefGoogle Scholar
  52. 52.
    Zhang JX et al (2016) In vitro establishment of a highly effective method of castor bean (Ricinus communis L.) regeneration using shoot explants. J Integr Agric 15(6):1417–1422CrossRefGoogle Scholar
  53. 53.
    Kumar S et al (2012) Biotechnological advances in jojoba Simmondsia chinensis (link) Schneider : recent developments and prospects for further research. Plant Biotechnol Rep 6(2):97–106CrossRefGoogle Scholar
  54. 54.
    Sood A, Chauhan RS (2015) Regulation of FA and TAG biosynthesis pathway genes in endosperms and embryos of high and low oil content genotypes of Jatropha curcas L. Plant Physiol Biochem 94:253–267PubMedCrossRefGoogle Scholar
  55. 55.
    Feldmann KA et al (1989) A dwarf mutant of arabidopsis generated by T-DNA insertion mutagenesis. Science 243(4896):1351–1354PubMedCrossRefGoogle Scholar
  56. 56.
    Kamthan A et al (2015) Small RNAs in plants: recent development and application for crop improvement. Front Plant Sci 6:208PubMedPubMedCentralCrossRefGoogle Scholar
  57. 57.
    Saurabh S, Vidyarthi AS, Prasad D (2014) RNA interference: concept to reality in crop improvement. Planta 239(3):543–564PubMedCrossRefGoogle Scholar
  58. 58.
    Rossak M, Smith M, Kunst L (2001) Expression of the FAE1 gene and FAE1 promoter activity in developing seeds of Arabidopsis thaliana. Plant Mol Biol 46(6):717–725PubMedCrossRefGoogle Scholar
  59. 59.
    Plant AL et al (1994) Regulation of an arabidopsis oleosin gene promoter in transgenic brassica-napus. Plant Mol Biol 25(2):193–205PubMedCrossRefGoogle Scholar
  60. 60.
    Guerche P et al (1990) Differential expression of the arabidopsis 2S albumin genes and the effect of increasing gene family size. Plant Cell 2(5):469–478PubMedPubMedCentralCrossRefGoogle Scholar
  61. 61.
    Shockey J et al (2015) Development and analysis of a highly flexible multi-gene expression system for metabolic engineering in Arabidopsis seeds and other plant tissues. Plant Mol Biol 89(1–2):113–126PubMedCrossRefGoogle Scholar
  62. 62.
    Butaye KMJ et al (2005) Approaches to minimize variation of transgene expression in plants. Mol Breed 16(1):79–91CrossRefGoogle Scholar
  63. 63.
    Gudynaite-Savitch L, Johnson DA, Miki BL (2009) Strategies to mitigate transgene-promoter interactions. Plant Biotechnol J 7(5):472–485PubMedCrossRefGoogle Scholar
  64. 64.
    Sidorenko LV et al (2017) GC-rich coding sequences reduce transposon-like, small RNA-mediated transgene silencing. Nat Plant 3:875–884CrossRefGoogle Scholar
  65. 65.
    van Erp H et al (2011) Castor phospholipid: diacylglycerol acyltransferase facilitates efficient metabolism of hydroxy fatty acids in transgenic arabidopsis. Plant Physiol 155(2):683–693PubMedCrossRefGoogle Scholar
  66. 66.
    Yu XH et al (2014) Coexpressing Escherichia coli cyclopropane synthase with sterculia foetida lysophosphatidic acid acyltransferase enhances cyclopropane fatty acid accumulation. Plant Physiol 164(1):455–465PubMedCrossRefGoogle Scholar
  67. 67.
    Zhang K et al (2017) Progress in genome editing technology and its application in plants. Front Plant Sci 8:177PubMedPubMedCentralGoogle Scholar
  68. 68.
    Rani R et al (2016) CRISPR/Cas9: a promising way to exploit genetic variation in plants. Biotechnol Lett 38(12):1991–2006PubMedCrossRefGoogle Scholar
  69. 69.
    Petolino JF, Srivastava V, Daniell H (2016) Editing plant genomes: a new era of crop improvement. Plant Biotechnol J 14(2):435–436PubMedCrossRefGoogle Scholar
  70. 70.
    van de Wiel CCM et al (2017) New traits in crops produced by genome editing techniques based on deletions. Plant Biotechnol Rep 11(1):1–8PubMedPubMedCentralCrossRefGoogle Scholar
  71. 71.
    Webb SR et al (2013) The EXZACT (TM) precision transformation & gene stacking platform: design, development, deployment and implications on new plant product discovery and development. In Vitro Cell Dev Biol Anim 49:S14–S14CrossRefGoogle Scholar
  72. 72.
    Ainley WM et al (2013) Trait stacking via targeted genome editing. Plant Biotechnol J 11(9):1126–1134PubMedCrossRefGoogle Scholar
  73. 73.
    Demorest ZL et al (2016) Direct stacking of sequence-specific nuclease-induced mutations to produce high oleic and low linolenic soybean oil. BMC Plant Biol 16:8CrossRefGoogle Scholar
  74. 74.
    Jiang WZ et al (2017) Significant enhancement of fatty acid composition in seeds of the allohexaploid, Camelina sativa, using CRISPR/Cas9 gene editing. Plant Biotechnol J 15(5):648–657PubMedPubMedCentralCrossRefGoogle Scholar
  75. 75.
    Aznar-Moreno JA, Durrett TP (2017) Simultaneous targeting of multiple gene homeologs to alter seed oil production in Camelina sativa. Plant Cell Physiol 58(7):1260–1267PubMedCrossRefGoogle Scholar
  76. 76.
    Gupta M et al (2012) Transcriptional activation of Brassica napus beta-ketoacyl-ACP synthase II with an engineered zinc finger protein transcription factor. Plant Biotechnol J 10(7):783–791PubMedCrossRefGoogle Scholar
  77. 77.
    Hammad S, Pu SH, Jones PJ (2016) Current evidence supporting the link between dietary fatty acids and cardiovascular disease. Lipids 51(5):507–517PubMedCrossRefGoogle Scholar
  78. 78.
    Jakobsen MU et al (2009) Major types of dietary fat and risk of coronary heart disease: a pooled analysis of 11 cohort studies. Am J Clin Nutr 89(5):1425–1432PubMedPubMedCentralCrossRefGoogle Scholar
  79. 79.
    Simopoulos AP, DiNicolantonio JJ (2016) The importance of a balanced ω-6 to ω-3 ratio in the prevention and management of obesity. Open Heart 3(2):e000385PubMedPubMedCentralCrossRefGoogle Scholar
  80. 80.
    Salas JJ, Ohlrogge JB (2002) Characterization of substrate specificity of plant FatA and FatB acyl-ACP thioesterases. Arch Biochem Biophys 403(1):25–34PubMedCrossRefGoogle Scholar
  81. 81.
    Zhang P et al (2008) Mutations in a delta(9)-stearoyl-ACP-desaturase gene are associated with enhanced stearic acid levels in soybean seeds. Crop Sci 48(6):2305–2313CrossRefGoogle Scholar
  82. 82.
    Knutzon DS et al (1992) Modification of brassica seed oil by antisense expression of a stearoyl-acyl carrier protein desaturase gene. Proc Natl Acad Sci U S A 89(7):2624–2628PubMedPubMedCentralCrossRefGoogle Scholar
  83. 83.
    Cardinal AJ et al (2007) Molecular analysis of soybean lines with low palmitic acid content in the seed oil. Crop Sci 47(1):304–310CrossRefGoogle Scholar
  84. 84.
    Li L et al (2011) An 11-bp insertion in Zea mays fatb reduces the palmitic acid content of fatty acids in maize grain. PLoS One 6(9):e24699PubMedPubMedCentralCrossRefGoogle Scholar
  85. 85.
    Zheng Honggang, F.C.C.O.U.S., et al. (2013) Brassica plants yielding oils with a low total saturated fatty acid content. USGoogle Scholar
  86. 86.
    Bonaventure G et al (2003) Disruption of the FATB gene in Arabidopsis demonstrates an essential role of saturated fatty acids in plant growth. Plant Cell 15(4):1020–1033PubMedPubMedCentralCrossRefGoogle Scholar
  87. 87.
    Dormann P, Voelker TA, Ohlrogge JB (2000) Accumulation of palmitate in arabidopsis mediated by the acyl-acyl carrier protein thioesterase FATB1. Plant Physiol 123(2):637–643PubMedPubMedCentralCrossRefGoogle Scholar
  88. 88.
    Belide S et al (2012) Modification of seed oil composition in arabidopsis by artificial microrna-mediated gene silencing. Front Plant Sci 3:168PubMedPubMedCentralCrossRefGoogle Scholar
  89. 89.
    Hawkins DJ, Kridl JC (1998) Characterization of acyl-ACP thioesterases of mangosteen (Garcinia mangostana) seed and high levels of stearate production in transgenic canola. Plant J 13(6):743–752PubMedCrossRefGoogle Scholar
  90. 90.
    Knutzon DS et al (1999) Lysophosphatidic acid acyltransferase from coconut endosperm mediates the insertion of laurate at the sn-2 position of triacylglycerols in lauric rapeseed oil and can increase total laurate levels. Plant Physiol 120(3):739–746PubMedPubMedCentralCrossRefGoogle Scholar
  91. 91.
    Pidkowich MS et al (2007) Modulating seed beta-ketoacyl-acyl carrier protein synthase II level converts the composition of a temperate seed oil to that of a palm-like tropical oil. Proc Natl Acad Sci U S A 104(11):4742–4747PubMedPubMedCentralCrossRefGoogle Scholar
  92. 92.
    James DW, Dooner HK (1991) Novel seed lipid phenotypes in combinations of mutants altered in fatty-acid biosynthesis in arabidopsis. Theor Appl Genet 82(4):409–412PubMedCrossRefGoogle Scholar
  93. 93.
    Carlsson AS et al (2002) A KAS2 cDNA complements the phenotypes of the Arabidopsis fab1 mutant that differs in a single residue bordering the substrate binding pocket. Plant J 29(6):761–770PubMedCrossRefGoogle Scholar
  94. 94.
    Liu Q et al (2017) Genetic enhancement of palmitic acid accumulation in cotton seed oil through RNAi down-regulation of ghKAS2 encoding beta-ketoacyl-ACP synthase II (KASII). Plant Biotechnol J 15(1):132–143PubMedCrossRefGoogle Scholar
  95. 95.
    Kinney AJ (1996) Beta-ketoacyl-ACP synthetase II genes from plants. E.I.D.P.d. Nemours, et al. (ed). USGoogle Scholar
  96. 96.
    Rubin Wilson BC, Young SA, Folkerts O (2001) Nucleotide sequences of maize and soybean beta-ketoacyl-acyl carrier protein synthase II and their use in the regulation of fatty acid content of oil, I.I.N. Dow AgroSciences Llc (ed). USGoogle Scholar
  97. 97.
    Gupta M et al (2012) Transcriptional activation of Brassica napus ss-ketoacyl-ACP synthase II with an engineered zinc finger protein transcription factor. Plant Biotechnol J 10(7):783–791PubMedCrossRefGoogle Scholar
  98. 98.
    Dehesh K et al (2001) Overexpression of 3-ketoacyl-acyl-carrier protein synthase IIIs in plants reduces the rate of lipid synthesis. Plant Physiol 125(2):1103–1114PubMedPubMedCentralCrossRefGoogle Scholar
  99. 99.
    Primomo VS et al (2002) Genotype X environment interactions, stability, and agronomic performance of soybean with altered fatty acid profiles. Crop Sci 42(1):37–44PubMedCrossRefGoogle Scholar
  100. 100.
    Delaney B et al (2008) Subchronic feeding study of high oleic acid soybeans (event DP-3Ø5423-1) in Sprague–Dawley rats. Food Chem Toxicol 46(12):3808–3817PubMedCrossRefGoogle Scholar
  101. 101.
    Flores T et al (2008) Silencing of GmFAD3 gene by siRNA leads to low alpha-linolenic acids (18:3) of fad3-mutant phenotype in soybean [Glycine max (Merr.)]. Transgenic Res 17(5):839–850PubMedCrossRefGoogle Scholar
  102. 102.
    Morineau C et al (2017) Selective gene dosage by CRISPR-Cas9 genome editing in hexaploid Camelina sativa. Plant Biotechnol J 15(6):729–739PubMedPubMedCentralCrossRefGoogle Scholar
  103. 103.
    Eckert H et al (2006) Co-expression of the borage Delta 6 desaturase and the Arabidopsis Delta 15 desaturase results in high accumulation of stearidonic acid in the seeds of transgenic soybean. Planta 224(5):1050–1057PubMedCrossRefGoogle Scholar
  104. 104.
    Ruiz-Lopez N et al (2009) The synthesis and accumulation of stearidonic acid in transgenic plants: a novel source of 'heart-healthy' omega-3 fatty acids. Plant Biotechnol J 7(7):704–716PubMedCrossRefGoogle Scholar
  105. 105.
    Ulmasov T et al (2012) High-oleic, low-saturate soybeans offer a sustainable and nutritionally enhanced solution for food applications requiring high oil stability A2 - Wilson, Richard F. In: Designing soybeans for 21st century markets. AOCS Press, Urbana, pp 277–295CrossRefGoogle Scholar
  106. 106.
    Liu Q, Singh S, Green A (2002) High-oleic and high-stearic cottonseed oils: nutritionally improved cooking oils developed using gene silencing. J Am Coll Nutr 21(3):205S–211SPubMedCrossRefGoogle Scholar
  107. 107.
    Liu Q, Singh S, Green A (2000) Genetic modification of cotton seed oil using inverted-repeat gene-silencing techniques. Biochem Soc Trans 28:927–929PubMedCrossRefGoogle Scholar
  108. 108.
    Liu F et al (2017) Simultaneous silencing of GhFAD2-1 and GhFATB enhances the quality of cottonseed oil with high oleic acid. J Plant Physiol 215:132–139PubMedCrossRefGoogle Scholar
  109. 109.
    Park H et al (2014) Stacking of a stearoyl-ACP thioesterase with a dual-silenced palmitoyl-ACP thioesterase and Δ12 fatty acid desaturase in transgenic soybean. Plant Biotechnol J 12(8):1035–1043PubMedCrossRefGoogle Scholar
  110. 110.
    Sun J-Y et al (2014) Simultaneous over-expressing of an acyl-ACP thioesterase (FatB) and silencing of acyl-acyl carrier protein desaturase by artificial microRNAs increases saturated fatty acid levels in Brassica napus seeds. Plant Biotechnol J 12(5):624–637CrossRefGoogle Scholar
  111. 111.
    Nguyen HT et al (2010) Metabolic engineering of seeds can achieve levels of omega-7 fatty acids comparable with the highest levels found in natural plant sources. Plant Physiol 154(4):1897–1904PubMedPubMedCentralCrossRefGoogle Scholar
  112. 112.
    Fahy D et al (2013) Reducing saturated fatty acids in Arabidopsis seeds by expression of a Caenorhabditis elegans 16:0-specific desaturase. Plant Biotechnol J 11(4):480–489PubMedCrossRefGoogle Scholar
  113. 113.
    Nguyen HT et al (2015) Redirection of metabolic flux for high levels of omega-7 monounsaturated fatty acid accumulation in camelina seeds. Plant Biotechnol J 13(1):38–50PubMedCrossRefGoogle Scholar
  114. 114.
    Haslam RP et al (2012) The modification of plant oil composition via metabolic engineering-better nutrition by design. Plant Biotechnol J 11(2):157–168PubMedCrossRefGoogle Scholar
  115. 115.
    Ruiz-Lopez N et al (2012) Metabolic engineering of the omega-3 long chain polyunsaturated fatty acid biosynthetic pathway into transgenic plants. J Exp Bot 63(7):2397–2410PubMedCrossRefGoogle Scholar
  116. 116.
    Ruiz-Lopez N et al (2013) Reconstitution of EPA and DHA biosynthesis in Arabidopsis: iterative metabolic engineering for the synthesis of n−3 LC-PUFAs in transgenic plants. Metab Eng 17:30–41PubMedPubMedCentralCrossRefGoogle Scholar
  117. 117.
    Petrie JR et al (2012) Metabolic engineering plant seeds with fish oil-like levels of DHA. PLoS One 7(11):e49165PubMedPubMedCentralCrossRefGoogle Scholar
  118. 118.
    Sayanova O et al (2012) The role of Delta6-desaturase acyl-carrier specificity in the efficient synthesis of long-chain polyunsaturated fatty acids in transgenic plants. Plant Biotechnol J 10(2):195–206PubMedCrossRefGoogle Scholar
  119. 119.
    Petrie JR et al (2014) Metabolic engineering Camelina sativa with fish oil-like levels of DHA. PLoS One 9(1):e85061PubMedPubMedCentralCrossRefGoogle Scholar
  120. 120.
    Ruiz-Lopez, N., et al. (2013) Successful high-level accumulation of fish oil omega-3 long-chain polyunsaturated fatty acids in a transgenic oilseed crop. The Plant JournalGoogle Scholar
  121. 121.
    Usher S et al (2017) Tailoring seed oil composition in the real world: optimising omega-3 long chain polyunsaturated fatty acid accumulation in transgenic Camelina sativa. Sci Rep 7(1):6570PubMedPubMedCentralCrossRefGoogle Scholar
  122. 122.
    Metz JG et al (2001) Production of polyunsaturated fatty acids by polyketide synthases in both prokaryotes and eukaryotes. Science 293(5528):290–293PubMedCrossRefGoogle Scholar
  123. 123.
    Barclay W, Weaver C, Metz J (2005) Development of a docosahexaenoic acid production technology using schizochytrium. In Single cell oils. AOCS PublishingGoogle Scholar
  124. 124.
    Hauvermale A et al (2006) Fatty acid production in Schizochytrium sp.: involvement of a polyunsaturated fatty acid synthase and a type I fatty acid synthase. Lipids 41(8):739–747PubMedCrossRefGoogle Scholar
  125. 125.
    Walsh TA, et al. (2016) Canola engineered with a microalgal polyketide synthase-like system produces oil enriched in docosahexaenoic acid. Nat Biotech. Advance online publicationGoogle Scholar
  126. 126.
    Ruiz-Lopez N et al (2013) Successful high-level accumulation of fish oil omega-3 long chain polyunsaturated fatty acids in a transgenic oilseed crop. Plant J 77(2):198–208PubMedPubMedCentralCrossRefGoogle Scholar
  127. 127.
    Broun P, Somerville C (1997) Accumulation of ricinoleic, lesquerolic, and densipolic acids in seeds of transgenic Arabidopsis plants that express a fatty acyl hydroxylase cDNA from castor bean. Plant Physiol 113(3):933–942PubMedPubMedCentralCrossRefGoogle Scholar
  128. 128.
    Smith MA et al (2003) Heterologous expression of a fatty acid hydroxylase gene in developing seeds of Arabidopsis thaliana. Planta 217(3):507–516PubMedCrossRefGoogle Scholar
  129. 129.
    Burgal J et al (2008) Metabolic engineering of hydroxy fatty acid production in plants: RcDGAT2 drives dramatic increases in ricinoleate levels in seed oil. Plant Biotechnol J 6(8):819–831PubMedPubMedCentralCrossRefGoogle Scholar
  130. 130.
    van Erp H et al (2015) Reducing isozyme competition increases target fatty acid accumulation in seed triacylglycerols of transgenic arabidopsis. Plant Physiol 168(1):36–46PubMedPubMedCentralCrossRefGoogle Scholar
  131. 131.
    Bayon S et al (2015) A small phospholipase A2-alpha from castor catalyzes the removal of hydroxy fatty acids from phosphatidylcholine in transgenic Arabidopsis seeds. Plant Physiol 167(4):1259–1270PubMedPubMedCentralCrossRefGoogle Scholar
  132. 132.
    Wayne LL, Browse J (2013) Homologous electron transport components fail to increase fatty acid hydroxylation in transgenic Arabidopsis thaliana. F1000Res 2:203PubMedPubMedCentralGoogle Scholar
  133. 133.
    Bates PD, Browse J (2011) The pathway of triacylglycerol synthesis through phosphatidylcholine in Arabidopsis produces a bottleneck for the accumulation of unusual fatty acids in transgenic seeds. Plant J 68(3):387–399PubMedCrossRefGoogle Scholar
  134. 134.
    Bates PD et al (2012) Acyl editing and headgroup exchange are the major mechanisms that direct polyunsaturated fatty acid flux into triacylglycerols. Plant Physiol 160(3):1530–1539PubMedPubMedCentralCrossRefGoogle Scholar
  135. 135.
    Bates PD et al (2014) Fatty acid synthesis is inhibited by inefficient utilization of unusual fatty acids for glycerolipid assembly. Proc Natl Acad Sci U S A 111(3):1204–1209PubMedPubMedCentralCrossRefGoogle Scholar
  136. 136.
    Broadwater JA, Whittle E, Shanklin J (2002) Desaturation and hydroxylation. Residues 148 and 324 of Arabidopsis FAD2, in addition to substrate chain length, exert a major influence in partitioning of catalytic specificity. J Biol Chem 277(18):15613–15620PubMedCrossRefGoogle Scholar
  137. 137.
    Dyer JM et al (2002) Molecular analysis of a bifunctional fatty acid conjugase/desaturase from tung. Implications for the evolution of plant fatty acid diversity. Plant Physiol 130(4):2027–2038PubMedPubMedCentralCrossRefGoogle Scholar
  138. 138.
    Lee M et al (1998) Identification of non-heme diiron proteins that catalyze triple bond and epoxy group formation. Science 280(5365):915–918PubMedCrossRefGoogle Scholar
  139. 139.
    Cahoon EB et al (2006) Conjugated fatty acids accumulate to high levels in phospholipids of metabolically engineered soybean and Arabidopsis seeds. Phytochemistry 67(12):1166–1176PubMedCrossRefGoogle Scholar
  140. 140.
    Mietkiewska E et al (2014) Combined transgenic expression of Punica granatum conjugase (FADX) and FAD2 desaturase in high linoleic acid Arabidopsis thaliana mutant leads to increased accumulation of punicic acid. Planta 240(3):575–583PubMedCrossRefGoogle Scholar
  141. 141.
    Singh S et al (2000) Inhibition of polyunsaturated fatty acid accumulation in plants expressing a fatty acid epoxygenase. Biochem Soc Trans 28(6):940–942PubMedCrossRefGoogle Scholar
  142. 142.
    Singh S et al (2001) Transgenic expression of a delta 12-epoxygenase gene in Arabidopsis seeds inhibits accumulation of linoleic acid. Planta 212(5–6):872–879PubMedCrossRefGoogle Scholar
  143. 143.
    Rezzonico E et al (2004) Level of accumulation of epoxy fatty acid in Arabidopsis thaliana expressing a linoleic acid delta12-epoxygenase is influenced by the availability of the substrate linoleic acid. Theor Appl Genet 109(5):1077–1082PubMedCrossRefGoogle Scholar
  144. 144.
    Li R et al (2010) Vernonia DGATs increase accumulation of epoxy fatty acids in oil. Plant Biotechnol J 8(2):184–195PubMedCrossRefGoogle Scholar
  145. 145.
    Li R et al (2012) Vernonia DGATs can complement the disrupted oil and protein metabolism in epoxygenase-expressing soybean seeds. Metab Eng 14(1):29–38PubMedCrossRefGoogle Scholar
  146. 146.
    Yu XH et al (2018) Identification of bottlenecks in the accumulation of cyclic fatty acids in camelina seed oil. Plant Biotechnol J 16:926–938PubMedPubMedCentralCrossRefGoogle Scholar
  147. 147.
    Zhu LH et al (2016) Dedicated industrial oilseed crops as metabolic engineering platforms for sustainable industrial feedstock production. Sci Rep 6:22181PubMedPubMedCentralCrossRefGoogle Scholar
  148. 148.
    Ruiz-Lopez N et al (2017) Tailoring the composition of novel wax esters in the seeds of transgenic Camelina sativa through systematic metabolic engineering. Plant Biotechnol J 15(7):837–849PubMedPubMedCentralCrossRefGoogle Scholar
  149. 149.
    Roesler K et al (2016) An improved variant of soybean type 1 diacylglycerol acyltransferase increases the oil content and decreases the soluble carbohydrate content of soybeans. Plant Physiol 171(2):878–893PubMedPubMedCentralGoogle Scholar
  150. 150.
    Ichihara Ki, Takahashi T (1988) Fujii, Diacylglycerol acyltransferase in maturing safflower seeds: its influences on the fatty acid composition of triacylglycerol and on the rate of triacylglycerol synthesis. Biochim Biophys Acta 958(1):125–129PubMedCrossRefGoogle Scholar
  151. 151.
    Hobbs DH, Lu C, Hills MJ (1999) Cloning of a cDNA encoding diacylglycerol acyltransferase from Arabidopsis thaliana and its functional expression. FEBS Lett 452(3):145–149PubMedCrossRefGoogle Scholar
  152. 152.
    Routaboul JM et al (1999) The TAG1 locus of Arabidopsis encodes for a diacylglycerol acyltransferase. Plant Physiol Biochem 37(11):831–840PubMedCrossRefGoogle Scholar
  153. 153.
    Zou JT et al (1999) The Arabidopsis thaliana TAG1 mutant has a mutation in a diacylglycerol acyltransferase gene. Plant J 19(6):645–653PubMedCrossRefGoogle Scholar
  154. 154.
    Lardizabal KD et al (2001) DGAT2 is a new diacylglycerol acyltransferase gene family: purification, cloning, and expression in insect cells of two polypeptides from Mortierella ramanniana with diacylglycerol acyltransferase activity. J Biol Chem 276(42):38862–38869PubMedCrossRefGoogle Scholar
  155. 155.
    Shockey JM et al (2006) Tung tree DGAT1 and DGAT2 have nonredundant functions in triacylglycerol biosynthesis and are localized to different subdomains of the endoplasmic reticulum. Plant Cell 18(9):2294–2313PubMedPubMedCentralCrossRefGoogle Scholar
  156. 156.
    Jako C et al (2001) Seed-specific over-expression of an Arabidopsis cDNA encoding a diacylglycerol acyltransferase enhances seed oil content and seed weight. Plant Physiol 126(2):861–874PubMedPubMedCentralCrossRefGoogle Scholar
  157. 157.
    Taylor DC et al (2009) Molecular modification of triacylglycerol accumulation by over-expression of DGAT1 to produce canola with increased seed oil content under field conditions. Botany-Botanique 87(6):533–543CrossRefGoogle Scholar
  158. 158.
    Weselake RJ et al (2008) Metabolic control analysis is helpful for informed genetic manipulation of oilseed rape (Brassica napus) to increase seed oil content. J Exp Bot 59(13):3543–3549PubMedPubMedCentralCrossRefGoogle Scholar
  159. 159.
    Chen G et al (2017) High-performance variants of plant diacylglycerol acyltransferase 1 generated by directed evolution provide insights into structure function. Plant J 92(2):167–177PubMedCrossRefGoogle Scholar
  160. 160.
    Lardizabal K et al (2008) Expression of <em>Umbelopsis ramanniana DGAT2A</em> in seed increases oil in soybean. Plant Physiol 148(1):89–96PubMedPubMedCentralCrossRefGoogle Scholar
  161. 161.
    Liu J et al (2010) Increasing seed mass and oil content in transgenic Arabidopsis by the overexpression of wri1-like gene from Brassica napus. Plant Physiol Biochem 48(1):9–15PubMedCrossRefGoogle Scholar
  162. 162.
    Liu FS et al (2016) Modification of starch metabolism in transgenic Arabidopsis thaliana increases plant biomass and triples oilseed production. Plant Biotechnol J 14(3):976–985PubMedCrossRefGoogle Scholar
  163. 163.
    Vanhercke T et al (2014) Metabolic engineering of biomass for high energy density: oilseed-like triacylglycerol yields from plant leaves. Plant Biotechnol J 12(2):231–239PubMedCrossRefGoogle Scholar
  164. 164.
    Vanhercke T et al (2017) Step changes in leaf oil accumulation via iterative metabolic engineering. Metab Eng 39:237–246PubMedCrossRefGoogle Scholar
  165. 165.
    El Tahchy A et al (2017) Thioesterase overexpression in Nicotiana benthamiana leaf increases the fatty acid flux into triacylgycerol. FEBS Lett 591(2):448–456PubMedCrossRefGoogle Scholar
  166. 166.
    Yurchenko O et al (2017) Engineering the production of conjugated fatty acids in Arabidopsis thaliana leaves. Plant Biotechnol J 15(8):1010–1023PubMedPubMedCentralCrossRefGoogle Scholar
  167. 167.
    Fouillen L, Colsch B, Lessire R(2013) The lipid world concept of plant lipidomics. In Metabolomics coming of age with its technological diversity, Rolin D (Ed). p. 331–76Google Scholar
  168. 168.
    Horn PJ, Chapman KD (2014) Lipidomics in situ: insights into plant lipid metabolism from high resolution spatial maps of metabolites. Prog Lipid Res 54:32–52PubMedCrossRefGoogle Scholar
  169. 169.
    Alonso AP, Val DL, Shachar-Hill Y (2011) Understanding fatty acid synthesis in developing maize embryos using metabolic flux analysis. Metab Eng 13(4):454–454CrossRefGoogle Scholar
  170. 170.
    Tan G-Y, Liu T (2017) Rational synthetic pathway refactoring of natural products biosynthesis in actinobacteria. Metab Eng 39(Supplement C):228–236PubMedCrossRefGoogle Scholar
  171. 171.
    CropLife International (2011) Cost of bringing a biotech crop to market. Accessed 11 Jun 2017

Copyright information

© Springer Science+Business Media, LLC, part of Springer Nature 2019

Authors and Affiliations

  • Laura L. Wayne
    • 1
  • Daniel J. Gachotte
    • 2
  • Terence A. Walsh
    • 2
  1. 1.Corteva Agriscience™Agriculture Division of DowDuPont™JohnstonUSA
  2. 2.Corteva Agriscience™Agriculture Division of DowDuPont™IndianapolisUSA

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