Abstract
The demand for the production of valuable secondary metabolites is increasing rapidly. While many metabolites can be directly extracted from intact plants, others are routinely produced using cell or organ cultures. The latter, also called Hairy roots when generated through the transformation with the bacterium Agrobacterium rhizogenes, are also amenable to molecular modifications. Similar to intact plants metabolic pathways can be altered by introducing homologous or foreign genes. The better the knowledge of a given pathway, the more efficient will be the genetic alteration. Some of the general requirements for metabolic engineering of secondary metabolites will be discussed together with methodological considerations, especially the analysis of secondary metabolites and also the transformation methods. In addition, some examples for successful establishment of transgenic plants for metabolite production will be described. Finally, some alternative plant production systems will be discussed.
Access this chapter
Tax calculation will be finalised at checkout
Purchases are for personal use only
Abbreviations
- AGO:
-
Argonaute
- BL-SOM:
-
Batch-learning self-organizing map analysis
- DCL:
-
Dicer-like
- DSB:
-
Double stranded DNA breaks
- ER:
-
Endoplasmic reticulum
- GC:
-
Gas chromatography
- GMO:
-
Genetically modified organism
- GSL:
-
Glucosinolate
- HCA:
-
Hierarchical cluster analysis
- HPLC:
-
High performance liquid chromatography
- IEE:
-
Intercistronic expression element
- IR:
-
Infrared
- JA:
-
Jasmonic acid
- JA-Ile:
-
JA-Isoleucine
- LC:
-
Liquid chromatography
- MEP:
-
Methylerythritol-phosphate
- miRNA:
-
microRNA
- MS:
-
Mass spectrometry
- MVA:
-
Mevalonate
- NMR:
-
Nuclear magnetic resonance
- PA:
-
Pyrrolizidine alkaloid
- PCA:
-
Principal component analysis
- PLS-DA:
-
Partial least squares discriminant analysis
- QTL:
-
Quantitative Trait Loci
- RISC:
-
RNA-induced silencing complex
- SCF:
-
SKP, CUL, F-box
- TALEN:
-
Transcription activator-like effector nuclease
- Ti:
-
Tumor-inducing
- ZNF:
-
Zinc finger nuclease
References
Verpoorte R, Contin A, Memelink J (2002) Biotechnology for the production of plant secondary metabolites. Phytochem Rev 1:31–50
Gómez-Galera S, Pelacho AM, Gené A, Capell T, Christou P (2007) The genetic manipulation of medicinal and aromatic plants. Plant Cell Rep 26:1689–1715
Bogers RJ, Craker LE, Lange D (eds) (2006) Medicinal and aromatic plants: agricultural, commercial, ecological, legal, pharmacological, and social aspects. Springer, Dordrecht
Verpoorte R, Alfermann AW (eds) (2000) Metabolic engineering of plant secondary metabolism. Kluwer, Dordrecht
Chandra S, Chandra R (2011) Engineering secondary metabolite production in hairy roots. Phytochem Rev 10:371–395
Georgiev MI, Ludwig-Müller J, Bley T (2010) Hairy root culture: copying nature in new bioprocesses. In: Arora R (ed) Medicinal plant biotechnology. CAB International, Oxon, pp 156–175
Nitzsche A, Tokalov SV, Gutzeit HO, Ludwig-Müller J (2004) Chemical and biological characterization of cinnamic acid derivatives from cell cultures of lavender (Lavandula officinalis) induced by stress and jasmonic acid. J Agric Food Chem 52:2915–2923
Cannell RJP (ed) (1998) Natural products isolation. Methods in biotechnology, vol 4. Humana Press, Totowa
Matzke MA, Matzke AJM (1995) How and why do plants inactivate homologous (trans)genes? Plant Physiol 107:679–685
Sharp PM, Li W-H (1987) The codon adaptation index – a measure of directional synonymous codon usage bias, and its potential applications. Nucleic Acid Res 15:1281–1295
Cohen JD, Baldi BG, Slovin JP (1986) (13C6-[Benzene ring)-indole-3-acetic acid: a new internal standard for quantitative mass spectral analysis of indole-3-acetic acid in plants. Plant Physiol 80:14–19
Kim HK, Choi YH, Verpoorte R (2011) NMR-based plant metabolomics: where do we stand, where do we go? Trends Biotechnol 29:267–275
Okazaki Y, Saito K (2012) Recent advances of metabolomics in plant biotechnology. Plant Biotechnol Rep 6:1–15
Sawada H, Ieki H, Matsuda I (1995) PCR detection of Ti and Ri plasmids from phytopathogenic Agrobacterium strains. Appl Environ Microbiol 61:828–831
Grabkowska R, Krolicka A, Mielicki W, Wielanek M, Wysokinska H (2010) Genetic transformation of Harpagophytum procumbens by Agrobacterium rhizogenes: iridoid and phenylethanoid glycoside accumulation in hairy root cultures. Acta Physiol Plant 32:665–673
Georgiev M, Ludwig-Müller J, Alipieva K, Lippert A (2011) Sonication-assisted Agrobacterium rhizogenes-mediated transformation of Verbascum xanthophoeniceum Griseb. for bioactive metabolite accumulation. Plant Cell Rep 30:859–866
Scharff LB, Bock R (2013) Synthetic biology in plastids. Plant J 78:783–798
Bevan M (1984) Binary Agrobacterium vectors for plant transformation. Nucleic Acids Res 12:8711–8721
Zang Y-X, Kim D-H, Hong S-B (2008) Agrobacterium tumefaciens-mediated hairy root production from seedlings of Chinese cabbage. J Plant Biol 51:255–259
Azhagiri AK, Maliga P (2007) Exceptional paternal inheritance of plastids in Arabidopsis suggests that low-frequency leakage of plastids via pollen may be universal in plants. Plant J 52:817–823
Ruf S, Karcher D, Bock R (2007) Determining the transgene containment level provided by chloroplast transformation. Proc Natl Acad Sci U S A 104:6998–7002
Lu Y, Rijzaani H, Karcher D, Ruf S, Bock R (2013) Efficient metabolic pathway engineering in transgenic tobacco and tomato plastids with synthetic multigene operons. Proc Natl Acad Sci U S A 110:E623–E632
Collakova E, DellaPenna D (2001) Isolation and functional analysis of homogentisate phytyltransferase from Synechocystis sp. PCC 6803 and Arabidopsis. Plant Physiol 127:1113–1124
Bock R (2013) Strategies for metabolic pathway engineering with multiple transgenes. Plant Mol Biol 83:21–31
Day A, Goldschmidt-Clermont M (2011) The chloroplast transformation toolbox: selectable markers and marker removal. Plant Biotechnol J 9:540–553
Maliga P, Bock R (2011) Plastid biotechnology: food, fuel, and medicine for the 21st century. Plant Physiol 155:1501–1510
Hooykaas PJJ (2000) Agrobacterium, a natural metabolic engineer of plants. In: Verpoorte R, Alfermann AW (eds) Metabolic engineering of plant secondary metabolism. Kluwer, Dordrecht, pp 51–67
Jouhikainen K, Lindgren L, Jokelainen T, Hiltunen R, Teeri TH, Oksman-Caldentey KM (1999) Enhancement of scopolamine production in Hyoscyamus muticus L. hairy root cultures by genetic engineering. Planta 208:545–551
Verpoorte R, van der Heijden R, Memelink J (2000) Genetic engineering of plant secondary metabolism. In: Verpoorte R, Alfermann AW (eds) Metabolic engineering of plant secondary metabolism. Kluwer, Dordrecht, pp 31–50
Sato F, Hashimoto T, Hachiya A, Tamura K-I, Choi K-B, Morishige T, Fujimoto H, Yamada Y (2001) Metabolic engineering of plant alkaloid biosynthesis. Proc Natl Acad Sci U S A 98:367–372
Galneder E, Rueffer M, Wanner G, Tabata M, Zenk MH (1988) Alternative final steps in berberine biosynthesis in Coptis japonica cell cultures. Plant Cell Rep 7:1–4
Breitenbach JP, Bai C, Rivera SM, Canela R, Capell T, Christou P, Zhu C, Sandmann G (2014) A novel carotenoid, 4-keto-α-carotene, as an unexpected by-product during genetic engineering of carotenogenesis in rice callus. Phytochemistry 98:85–91
Winkel BSJ (2004) Metabolic channelling in plants. Annu Rev Plant Biol 55:85–107
Facchini PJ, St-Pierre B (2005) Synthesis and trafficking of alkaloid biosynthetic enzymes. Curr Opin Plant Biol 8:657–666
Bender J, Celenza JL (2009) Indolic glucosinolates at the crossroads of tryptophan metabolism. Phytochem Rev 8:25–37
Bednarek P, Pislewska-Bednarek M, Svatos A, Schneider B, Doubsky J, Mansurova M, Humphry M, Consonni C, Panstruga R, Sanchez-Vallet A, Molina A, Schulze-Lefert P (2009) A glucosinolate metabolism pathway in living plant cells mediates broad-spectrum antifungal defense. Science 323:101–106
Clay NK, Adio AM, Denoux C, Jander G, Ausubel FM (2009) Glucosinolate metabolites required for an Arabidopsis innate immune response. Science 323:95–101
Zeng J, Lytle AK, Gage D, Johnson SJ, Zhan J (2013) Specific chlorination of isoquinolines by a fungal flavin-dependent halogenase. Bioorg Med Chem Lett 23:1001–1003
Neumann CS, Fujimori DG, Walsh CT (2008) Halogenation strategies in natural product biosynthesis. Chem Biol 15:99–109
Smith DRM, Grüschow S, Goss RJM (2013) Scope and potential of halogenases in biosynthetic applications. Curr Opin Chem Biol 17:276–283
Zehner S, Kotzsch A, Bister B, Süssmuth RD, Mendez C, Salas JA, van Pee K-H (2005) A regioselective tryptophan 5-halogenase is involved in pyrroindomycin biosynthesis in Streptomyces rugosporus LL-42D005. Chem Biol 12:445–452
Yeh E, Garneau S, Walsh CT (2005) Robust in vitro activity of RebF and RebH, a two component reductase/halogenase, generating 7-chlorotryptophan during rebeccamycin biosynthesis. Proc Natl Acad Sci U S A 102:3960–3965
Runguphan W, Qu X, O’Connor SE (2010) Integrating carbon–halogen bond formation into medicinal plant metabolism. Nature 468:461–464
Hibbert EG, Dalby PA (2005) Directed evolution strategies for improved enzymatic performance. Microb Cell Fact 4:29
Runguphan W, Glenn WS, O’Connor SE (2012) Redesign of a dioxygenase in morphine biosynthesis. Chem Biol 19:674–678
El-Sayed M, Verpoorte R (2007) Catharanthus terpenoid indole alkaloids: biosynthesis and regulation. Phytochem Rev 6:277–305
Georgiev M, Agostini E, Ludwig-Müller J, Xu J (2012) Genetically transformed roots: from plant disease to biotechnology. Trends Biotechnol 30:528–537
Runguphan W, Maresh JJ, O’Connor SE (2009) Silencing of tryptamine biosynthesis for production of nonnatural alkaloids in plant culture. Proc Natl Acad Sci U S A 106:13673–13678
Hartmann T, Witte L (1995) Pyrrolizidine alkaloids: chemical, biological and chemoecological aspects. In: Pelletier SW (ed) Alkaloids: chemical and biological perspectives, vol 9. Pergamon, Oxford, pp 55–233
Röder E (1995) Medicinal plants in Europe containing pyrrolizidine alkaloids. Pharmazie 50:83–98
Cen T, Mei N, Fu PP (2010) Genotoxicity of pyrrolizidine alkaloids. J Appl Toxicol 30:183–196
Smith NA, Singh SP, Wang M-B, Stoutjesdijk PA, Green AG, Waterhouse PM (2000) Total silencing by intron spliced hairpin RNAs. Nature 407:319–320
Ossowski S, Schwab R, Weigel D (2008) Gene silencing in plants using artificial microRNAs and other small RNAs. Plant J 53:674–690
Voytas DF (2013) Plant genome engineering with sequence-specific nucleases. Annu Rev Plant Biol 64:327–350
Reyon D, Tsai SQ, Khayter C, Foden JA, Sander JD, Joung JK (2012) FLASH assembly of TALENs for high-throughput genome editing. Nat Biotechnol 30:460–465
Huizing HJ, Pfauth EC, Malingri TM, Sietsma JH (1983) Regeneration of plants from tissue- and cell suspension cultures of Symphytum officinale L. and effect of in vitro culture on pyrrolizidine alkaloid production. Plant Cell Tiss Organ Cult 2:227–238
Yang CQ, Fang X, Wu XM, Mao YB, Wang LJ, Chen XY (2012) Transcriptional regulation of plant secondary metabolism. J Integr Plant Biol 54:703–712
Chiu L-W, Zhou X, Burke S, Wu X, Prior RL, Li L (2010) The purple cauliflower arises from activation of a MYB transcription factor. Plant Physiol 154:1470–1480
De Geyter N, Gholami A, Goormachtig S, Goossens A (2012) Transcriptional machineries in jasmonate-elicited plant secondary metabolism. Trends Plant Sci 17:349–359
Gigolashvili T, Berger B, Flügge U-I (2009) Specific and coordinated control of indolic and aliphatic glucosinolate biosynthesis by R2R3-MYB transcription factors in Arabidopsis thaliana. Phytochem Rev 8:3–13
Memelink J, Gantet P (2007) Transcription factors involved in terpenoid indole alkaloid biosynthesis in Catharanthus roseus. Phytochem Rev 6:353–362
Peebles CAM, Hughes EH, Shanks JV, San K-Y (2009) Transcriptional response of the terpenoid indole alkaloid pathway to the overexpression of ORCA3 along with jasmonic acid elicitation of Catharanthus roseus hairy roots over time. Metab Eng 11:76–86
Thines B, Katsir L, Melotto M, Niu Y, Mandaokar A, Liu G, He NK, Yang S, Howe GA, Browse J (2007) JAZ repressor proteins are targets of the SCF(COI1) complex during jasmonate signalling. Nature 448:661–665
Pauwels L, Goossens A (2011) The JAZ proteins: a crucial interface in the jasmonate signaling cascade. Plant Cell 23:3089–3100
Katsir L, Chung HS, Koo AJK, Howe GA (2008) Jasmonate signaling: a conserved mechanism of hormone sensing. Curr Opin Plant Biol 11:428–435
Nims E, Dubois CP, Roberts SC, Walker EL (2006) Expression profiling of genes involved in paclitaxel biosynthesis for targeted metabolic engineering. Metab Eng 8:385–394
Grotewold E (2001) Subcellular trafficking of phytochemicals. Recent Res Devel Plant Physiol 2:31–48
Nour-Eldin HH, Halkier BA (2013) The emerging field of transport engineering of plant specialized metabolites. Curr Opin Biotechnol 24:263–270
Hamill JD, Robins RJ, Parr AJ, Evans DM, Furze JM, Rhodes MJC (1990) Over-expressing a yeast ornithine decarboxylase gene in transgenic roots of Nicotiana rustica can lead to enhanced nicotine accumulation. Plant Mol Biol 15:27–38
Tabata H (2004) Paclitaxel production by plant-cell-culture technology. Adv Biochem Eng Biotechnol 87:1–23
Guerra-Bubb J, Croteau R, Williams RM (2012) The early stages of the biosynthesis of taxol: an interim report on the synthesis and identification of early pathway metabolites. Nat Prod Rep 29:683–696
Croteau R, Ketchum REB, Long RM, Kaspera R, Wildung MR (2006) Taxol biosynthesis and molecular genetics. Phytochem Rev 5:75–97
Malik S, Cusidó RM, Mirjalili MH, Moyano E, Palazón J, Bonfill M (2011) Production of the anticancer drug taxol in Taxus baccata suspension cultures: a review. Process Biochem 46:23–34
Cusidó RM, Vidal H, Gallego A, Abdoli M, Palazón J (2013) Biotechnological production of taxanes: a molecular approach. In: Muñoz-Torrero D, Cortés A, Mariño EL (eds) Recent advances in pharmaceutical sciences III, vol 3. Transworld Research Network, Trivandrum, pp 91–107
Onrubia M, Moyano E, Bonfill M, Cusidó RM, Goossens A, Palazón J (2011) Coronatine, a more powerful elicitor for inducing taxane biosynthesis in Taxus media cell cultures than methyl jasmonate. J Plant Physiol 170:211–219
Hezari M, Lewis NG, Croteau R (1995) Purification and characterization of taxa-4(5),11(12)-diene synthase from Pacific yew (Taxus brevifolia) that catalyzes the first committed step of taxol biosynthesis. Arch Biochem Biophys 322:437–444
Rohmer M (1999) The discovery of a mevalonate-independent pathway for isoprenoid biosynthesis in bacteria, algae and higher plants. Nat Prod Rep 16:565–574
Fahey JW, Zalcmann AT, Talalay P (2001) The chemical diversity and distribution of glucosinolates and isothiocyanates among plants. Phytochemistry 56:5–51
Halkier BA, Gershenzon J (2006) Biology and biochemistry of glucosinolates. Annu Rev Plant Biol 57:303–333
Giamoustaris A, Mithen R (1997) Glucosinolates and disease resistance in oilseed rape. Plant Pathol 46:271–275
Radojčić Redovniković I, Glivetić T, Delonga K, Vorkapić-Furač J (2008) Glucosinolates and their potential role in plant. Period Biol 110:297–309
Kastell A, Smetanska I, Ulrichs C, Cai Z, Mewis I (2013) Effects of phytohormones and jasmonic acid on glucosinolate content in hairy root cultures of Sinapis alba and Brassica rapa. Appl Biochem Biotechnol 169:624–635
Kastell A, Smetanska I, Schreiner M, Mewis I (2013) Hairy roots, callus, and mature plants of Arabidopsis thaliana exhibit distinct glucosinolate and gene expression profiles. Plant Cell Tiss Organ Cult 115:45–54
Baskar V, Gururani MA, Yu JW, Park SW (2012) Engineering glucosinolates in plants: current knowledge and potential uses. Appl Biochem Biotechnol 168:1694–1717
Zang Y-X, Kim J-H, Park Y-D, Kim D-H, Hong S-B (2008) Metabolic engineering of aliphatic glucosinolates in Chinese cabbage plants expressing Arabidopsis MAM1, CYP79F1, and CYP83A1. BMB Rep 41:472–478
Bak S, Olsen CE, Peteresen BL, Møller BL, Halkier BA (1999) Metabolic engineering of p-hydroxybenzyl glucosinolate in Arabidopsis by expression of the cyanogenic CYP79A1 from Sorghum bicolor. Plant J 20:663–671
Mikkelsen MD, Halkier BA (2003) Metabolic engineering of valine- and isoleucine-derived glucosinolates in Arabidopsis expressing CYP79D2 from cassava. Plant Physiol 131:773–779
Mikkelsen MD, Hansen CH, Wittstock U, Halkier BA (2000) Cytochrome P450 CYP79B2 from Arabidopsis catalyzes the conversion of tryptophan to indole-3-acetaldoxime, a precursor of indole glucosinolates and indole-3-acetic acid. J Biol Chem 275:33712–33717
Geu-Flores F, Olsen CE, Halkier BA (2009) Towards engineering glucosinolates into noncruciferous plants. Planta 229:261–270
Decker EL, Reski R (2008) Current achievements in the production of complex biopharmaceuticals with moss bioreactors. Bioprocess Biosyst Eng 31:3–9
Skjanes K, Rebours C, Lindblad P (2013) Potential for green microalgae to produce hydrogen, pharmaceuticals and other high value products in a combined process. Crit Rev Biotechnol 33:172–215
Homann PH (2003) Hydrogen metabolism of green algae: discovery and early research – a tribute to Hans Gaffron and his coworkers. Photosynth Res 76:93–103
Hannon M, Gimpel J, Tran M, Rasala B, Mayfield S (2010) Biofuels from algae: challenges and potential. Biofuels 1:763–784
Shimogawara K, Fujiwara S, Grossman A, Usuda H (1998) High-efficiency transformation of Chlamydomonas reinhardtii by electroporation. Genetics 148:1821–1828
Neupert J, Shao N, Lu Y, Bock R (2012) Genetic transformation of the model green alga Chlamydomonas reinhardtii. Methods Mol Biol 847:35–47
Kumar SV, Misquitta RW, Reddy VS, Rao BJ, Rajam MV (2004) Genetic transformation of the green alga – Chlamydomonas reinhardtii by Agrobacterium tumefaciens. Plant Sci 166:731–738
Purton S (2007) Tools and techniques for chloroplast transformation of Chlamydomonas. Adv Exp Med Biol 616:34–45
Tate JJ, Gutierrez-Wing T, Rusch KA, Benton MG (2013) The effects of plant growth substances and mixed cultures on growth and metabolite production of green algae Chlorella sp.: a review. J Plant Growth Regul 32:417–428
Chow K-C, Tung WL (1999) Electro transformation of Chlorella vulgaris. Plant Cell Rep 18:778–780
Cha TS, Yee W, Aziz A (2012) Assessment of factors affecting Agrobacterium-mediated genetic transformation of the unicellular green alga, Chlorella vulgaris. World J Microbiol Biotechnol 28:1771–1779
Dawson HN, Burlingame R, Cannons AC (1997) Stable transformation of Chlorella: rescue of nitrate reductase-deficient mutants with the nitrate reductase gene. Curr Microbiol 35:356–362
Reski R (1998) Physcomitrella and Arabidopsis: the David and Goliath of reverse genetics. Trends Plant Sci 3:209–210
Ludwig-Müller J, Jülke S, Bierfreund NM, Decker EL, Reski R (2009) Moss (Physcomitrella patens) GH3 proteins act in auxin homeostasis. New Phytol 181:323–338
Wiedemann G, Hermsen C, Melzer M, Büttner-Mainik A, Rennenberg H, Reski R, Kopriva S (2010) Targeted knock-out of a gene encoding sulfite reductase in the moss Physcomitrella patens affects gametophytic and sporophytic development. FEBS Lett 584:2271–2278
Khraiwesh B, Arif MA, Seumel GI, Ossowski S, Weigel D, Reski R, Frank W (2010) Transcriptional control of gene expression by microRNAs. Cell 140:111–122
Büttner-Mainik A, Parsons J, Jérôme H, Hartmann A, Lamer S, Schaaf A, Schlosser A, Zipfel PF, Reski R, Decker EL (2011) Production of biologically active recombinant human factor H in Physcomitrella. Plant Biotechnol J 9:373–383
Asakawa Y (2007) Biologically active compounds from bryophytes. Pure Appl Chem 79:557–580
Beike AK, Decker EL, Frank W, Lang D, Vervliet-Scheebaum M, Zimmer AD, Reski R (2010) Applied bryology – bryotechnology. Trop Bryol 31:22–32
Frahm J-P (2004) Recent developments of commercial products from bryophytes. Bryologist 107:277–283
Rosenstiel TN, Shortlidge EE, Melnychenko AN, Pankow JF, Eppley SM (2012) Sex-specific volatile compounds influence microarthropod-mediated fertilization of moss. Nature 489:431–433
Richter H, Lieberei R, Strnad M, Novak O, Gruz J, Rensing SA, Schwartzenberg VK (2012) Polyphenol oxidases in Physcomitrella – functional PPO1 knockout modulates cytokinin-dependent development in the moss Physcomitrella patens. J Exp Bot 63:5121–5135
Schwartzenberg VK, Schultze W, Kassner H (2004) The moss Physcomitrella patens releases a tetracyclic diterpene. Plant Cell Rep 22:780–786
Erxleben A, Gessler A, Vervliet-Scheebaum M, Reski R (2012) Metabolite profiling of the moss Physcomitrella patens reveals evolutionary conservation of osmoprotective substances. Plant Cell Rep 31:427–436
Decker EL, Reski R (2012) Glycoprotein production in moss bioreactors. Plant Cell Rep 31:453–460
Anterola A, Shanle E, Perroud P-F, Quatrano R (2009) Production of taxa-4(5),11(12)-diene by transgenic Physcomitrella patens. Transgen Res 18:655–660
Verpoorte R (2000) Secondary metabolism. In: Verpoorte R, Alfermann AW (eds) Metabolic engineering of plant secondary metabolism. Kluwer, Dordrecht, pp 1–29
Acknowledgments
Work in the author’s laboratory was funded by the European Union and the State of Saxony.
Author information
Authors and Affiliations
Corresponding author
Editor information
Editors and Affiliations
Rights and permissions
Copyright information
© 2014 Springer Science+Business Media Dordrecht
About this chapter
Cite this chapter
Ludwig-Müller, J. (2014). Metabolic Engineering of Selected Secondary Metabolites. In: Paek, KY., Murthy, H., Zhong, JJ. (eds) Production of Biomass and Bioactive Compounds Using Bioreactor Technology. Springer, Dordrecht. https://doi.org/10.1007/978-94-017-9223-3_21
Download citation
DOI: https://doi.org/10.1007/978-94-017-9223-3_21
Published:
Publisher Name: Springer, Dordrecht
Print ISBN: 978-94-017-9222-6
Online ISBN: 978-94-017-9223-3
eBook Packages: Biomedical and Life SciencesBiomedical and Life Sciences (R0)