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Pergamon Biotechnology Advances, Vol. 13, No. 3, pp. 425--453, 1995
C, opyrisht © 1995 Elsevier Science lno. Printed in Great Britai~ All rishts reserved
0734-9750/95 $29.00 + .00
0734-9750(95)02005-N
PLANT CELL AND TISSUE CULTURE: ALTERNATIVES FOR METABOLITE PRODUCTION
FRANK DICOSMO 12 and MASANARU MISAWA 2'3
1Department of Botany and ZlnJtitute of Biomedical Engineering, University of Toronto, Toronto, Canada MSS 3B2
JBIO INTERNATIONAL INC., Suite 420, 151 Bloor Street West, Toronto, Ontario, Canada MSS 1S4
ABSTRACT
Plant cell culture systems represent a potential renewable source of valuable medicinals, flavours, essences and colourants that cannot be produced by microbial cells or chemical syntheses. However, only a few cultures produce these compounds in commercially useful amounts. The low productivities are associated with our poor understanding of the biochemistry of these systems. Recent advances in molecular biology, enzymology, physiology and fermentation technology of plant cell cultures suggest that these systems will become a viable source of important natural products. This review examines the sate of the art of production of medicinal plant secondary metabolites by plant cell cultures.
KEY WORDS: Plant cell culture technology, secondary metabolites, pharmaceuticals, medicinal compounds.
INTRODUCTION
Plants produce biochemicals that are of importance in the healthcare, food, flavour and
cosmetics industries. Many pharmaceuticals are produced from the secondary metabolites
of plants. Examples are digitalis, L-DOPA, morphine, codeine, reserpine, and the
anticancer drugs vincristine, vinblastine and taxol used in treatment of ovarian and breast
cancers. Currently, these and many other natural products are produced solely from
massive quantities of whole plant parts. Often the source plants are cultivated in tropical
or subtropical, geographically remote, areas which are subject to political instability,
drought, disease and changing land use patterns and other environmental factors. In
425
426 F. DICOSMO and M. MISAWA
addition, the long cultivation periods between planting and harvesting make selection of
high-yielding strains difficult, thus resulting in expensive drugs. Cultivation periods may
range from several months to decades for the taxol yielding, Taxus brevifolia trees. In spite
of these difficulties and costs, the extraction of medicinals from cultivated plants or plants
in the wild continues because of a lack of credible alternatives.
Clearly, the development of alternative and complimentary methods to whole plant
extraction for the production of clinical medicines is an issue of considerable socio-
economic importance. These factors have generated considerable interest in the use of
plant cell culture technologies for the production of pharmaceuticals [2,11,13,17-
19,22,30,42,48,59] and other plant derived biochemicals [2,10,32,41]. Indeed, the plant cell
culture technology is now sufficiently advanced to allow for large quantities of relatively
homogeneous, undifferentiated cells to be produced. Plant cell and tissue culture systems
are complementary and may provide competitive metabolite production systems when
compared to whole plant extraction. Commercial production of plant natural products via
cell and tissue culture systems becomes viable when the product commands a price
exceeding about $1000/kg [75].
Several types of high-yielding tissue culture systems have been developed. These
include the cultivation of specific organ cultures, suspension cultured cells selected for high
productivity on production media and high-density culture [52,65,86,92]. Certain inorganic
and organic adjuvants stimulate product synthesis and/or accumulation, but product
accumulation is transient [16]. Immobilized cells show promise for increasing synthesis of
biochemicals; however, their benefits are only realized when the product is excreted into
the medium [43,67,80]. Such systems offer the possibility of commercialization for some
very expensive products only. For some high-value-added products the culture systems may
have to compete with total chemical and/or enzyme-mediated syntheses. For example, the
fascile synthesis of a-3', 4'-anhydrovinblastine can be achieved in industrially attractive
yields, with either ferric chloride mediated synthesis or by using peroxidase enzymes [cited
in 16]. The detailed analysis of the biochemistry of plant cell cultures will certainly allow
for improved manipulation of natural product biosynthesis [50]. The production of
secondary metabolites in large bioreactors is therefore an attractive alternative method for
high-value added biochemicals production, with the possibility of controlled production
according to demand [49,68]. Despite the obvious possibilities many problems remain to
PLANT CELL AND TISSUE CULTURE 427
be solved before plant cell culture methods are used for the industrial production of plant
metabolites.
Mitsui Petrochemical Industry Company in Japan was the first to produce a
pharmaceutical and dyestuff on commercial scale with the production of shikonin, valued
at $4,500/kg (Table 1). The company succeeded also in using plant cell culture
technologies to produce the pharmaceutical berberine at a yield of 3.5 g per litre of
culture fluid. In both these systems cultivation of the cells as high density cultures was
essential for productivity. Nitto Denko Company, also in Japan, has successfully cultivated
Panaxginseng cells in 20 m 3 bioreactors for biomass production. Other applications of cell
culture technologies for pharmaceutical production are highlighted in Table 1.
While large scale plant cell suspension cultures are expected to be suitable for
industrial production of plant-derived biochemicals, the production technology needs to
be further developed. Significant differences between microbial and plant cell cultures
mean that the methods developed for microbial systems may have to be modified [4].
Plant cells are sensitive to shear stresses because of their large size and the relatively
inflexible cell wall. For this and other reasons turbine impellers may not be suitable for
plant cell cultures; instead, airlift bioreactors are often recommended. Plant cell cultures
show relatively long growth cycles. Typical growth rates may range from 0.12 d -1 to 0.05
d-l ; thus, the typical doubling time of plant cell cultures is measured in days, as compared
to hours for microbial systems. In plant cells, the vacuole is usually the site of product
accumulation and extracellular product secretion is rare. This creates special problems for
downstream processing, as the cells must be collected and the product extracted. Indeed,
it would be beneficial to develop methods that would allow for product excretion directly
into the growth medium; this would facilitate recovery, permit recycling of the biomass and
perhaps recycling of some media.
Cultured plant cells usually produce low amounts and altered profiles of secondary
metabolites when compared with the intact plant. Production and product profiles may not
be stable, deteriorating ultimately to inactive cultures. The low product yields are yet to
be explained satisfactorily, but indicate metabolic blocks concerning specific enzyme
repression and activity. Nonetheless, significant progress has been made in culture yield
improvements as illustrated in Table 1.
428 F. DICOSMO and M. MISAWA
Table 1. Examples of plant cell culture methodologies for the production of metabolites.
Products Production System Reference
Vincamine, 3.3 g'L -1 Cell culture of Vinca minor Equivincamine, 0.9 g.L -t
Shikonin, 4 g.L -1
Berberine, 3.5 g.L -1
Ajmaline, 0.4 g.L -1 Raucaffricine, 1.2 g.L-1
Strictosidine, gram amounts
a-3',4'-anhydrovin- blastine, about 70% yield
a-3',4'-anhydrovin- blastine, about 70% yield; vinblastine, about 20% yield
Methyldigoxin, 505 g produced in 3 months
Cell culture of Lithospermum erythrohizon
Cell culture of Coptis japonica
Cell culture of Rauwolfia serpentina
Immobilized strictosidine synthase
Glucose oxidase and peroxidase mediated dimerization
FeCl3-mediated dimerization
Biotransformation of methyldigitoxin by Digitalis lanata cells
Farmitalia, Ger. Often. DE 3,902,980 August 17, 1989; Chem. Abs. 196670S, 1990.
Mitsui Petrochem., (see Fujita, Y. and Tabata, M. in Plant Cell and Tissue Culture, Alan R. Liss Inc. pp. 169- 185, 1987).
Mitsui Petrochem. J. Chem. Tech. Biotech. 46: 61-69, 1989.
Schiibel et al. Phytochem. 28: 419-494, 1989.
Pfitzner and Zenk, Planta Med. 46: 10-14, 1982.
DiCosmo, F. Progress bz Plant Celhdar and Molecular Biology [16].
Allelix Inc., Vukovic, J. and Goodbody, A.E., U.S. Pat. 4,778,885.
Alferman, A.W. et al. (in Primary and Secondary Metabolism in Plant Cell Cultures, Springer-Verlag, pp. 316-322, 1985).
The increased use of plant cell culture systems in recent years is perhaps due to an
improved understanding of the biochemistry of secondary metabolic pathways in
economically important plants. This trend is expected to increase as advances in plant
biotechnology surge on. This review is not intended to be exhaustive, rather specific
reference is made to certain areas with demonstrated potential for industrial application.
PLANT CELL AND TISSUE CULTURE 429
APPROACHES TO INCREASE PRODUCTIVITY
For plant cell culture systems to become economically viable, it is important to develop
methods that would allow for consistent generation of high yields of products from
cultured cells [9]. Several products are accumulated in cultured cells at a higher level than
found in intact plants. This is due to careful selection of productive cells and cultural
conditions (Table 2). For example, berberine by Coptis japonica [54], ginsenosides by
Panax ginseng [83], rosmarinic acid by Coleus blumei [82], shikonin by Lithospermum
etythrorhizon [79], diosgenin by Dioscorea [55], ubiquinone-10 by Nicotiana tabacum were
accumulated in much higher levels in cultured cells than in the intact plants [30]. The
general experience, however, is that plant cell cultures usually lose the ability to produce
secondary metabolites that are characteristic of the intact plant [18]. In order to obtain
yields in concentrations high enough for commercial exploitation, efforts have focused on
the stimulation of biosynthetic activities of cultured cells using various methods.
Table 2. Secondary metabolites produced in high levels by plant cell cultures.
Compound Plant Species Yield (% dry wt) Cell Culture Whole Plant
Shikonin Ginsenoside Anthraquinones Ajmalicine Rosmarinic acid Ubiquinone-10 Diosgenin Benzylisoquinoline
alkaloids Berberine Berberine Anthraquinones Anthraquinones Nicotine Bisoclaurine Tripdiolide
Lithospermum erythrorhizon 20 (s*) 1.5 Panax ginseng 27 (c) 4.5 Morinda citrifolia 18 (s) 2.2 Catharanthus roseus 1.0 (s) 0.3 Coleus blumeii 15 (s) 3 Nicotiana tabacum 0.036 (s) 0.0003 Dioscorea deltoides 2 (s) 2
Coptisjaponica 11 (s) 5-10 Thalictrurn mb~or 10 (s) 0.01 Coptis japonica 10 (s) 2--4 Galium verum 5.4 (s) 1.2 Galium aparbze 3.8 (s) 0.2 Nicotiana tabacum 3.4 (c) 2.0 Stephania cepharantha 2.3 (s) 0.8 Tripterygium wilfordii 0.05 (s) 0.001
*s = suspension; c = callus
430 F. DICOSMO and M. MISAWA
Optimization of Cultural Conditions
Physical optimization. Several chemical and physical parameters affecting culture growth
have been tested extensively with various plant cells. These parameters include media
components, phytohormones, pH, temperature, pO2, pCO2, agitation and light among
others. Manipulation of the physical aspects as well as the nutritional elements in a culture
is perhaps is the most fundamental approach for optimization of culture productivity.
Many reports and patents have discussed optimization of cultural conditions for improved
growth rates of cells and/or higher yield of desirable products. A few notable examples are
highlighted here. DiCosmo and Towers [18] summarized the effects of various culture
manipulations on secondary metabolite biosynthesis. Various well-known basal media for
the production of indole alkaloids have been tested; the results indicate that serpentine
accumulation depends on the composition of the medium used, as might be expected.
Among them, Murashige and Skoog (MS) formulation was recognized as superior for the
production of serpentine by Catharan thus roseus suspension. This is not always true for
other species in culture.
Sucrose and glucose are the preferred carbon source for plant tissue cultures;
although other carbohydrate sources are often used. The concentration of the carbon
source affects cell growth and yield of secondary metabolites in many cases. In general,
sucrose appears to be the preferred carbon source for cultured plant cell systems.
DiCosmo and Towers [18] provided a review of the effects of nutritional factors on plant
cell culture growth and product yield. Hormone, auxin and kinetin levels have shown the
most remarkable effects on growth and productivity of plant metabolites. Increased auxin
levels in cultures, such as 2,4-dichlorophenoyacetic acid (2,4-D) in the medium promotes
dedifferentiation of cells and diminishes the accumulation of secondary metabolites.
Indeed, auxins added to solid media stimulate callus induction, but for product synthesis
it may be advisable to use low levels or remove auxins. For example, cytokinins stimulated
alkaloid synthesis when auxin was removed from the medium of a cell line of Catharan thus
roseus. However, accumulation of L-DOPA by M a c u n a pruriens [11] was stimulated by
relatively high amounts of 2,4-D. In Catharan thus roseus increased levels of alkaloids are
produced by cells transferred to production media. Accumulation of alkaloids begins a few
days after cells are transferred to production media and the greatest specific yields are
reached after approximately 12 days. Berlin et al. [10] compared various strategies
designed to improve indole alkaloid biosynthesis in C. roseus.
PLANT CELL AND TISSUE CULTURE 431
Selection of high-producing strains. Plant cells in culture represent a heterogeneous
population in which physiological characteristics of individual plant cells are different. The
techniques used in selection and screening plant cell cultures for improved product
synthesis are described by Berlin and Sasse [9]. Cell cloning methods provide a promising
way of selecting cell lines yielding increased levels of product. Most selection methods are
based on production of pigments, such as anthocyanins, betacyanins and others. A strain
of Euphorbia milli also accumulated about 7-fold the level of anthocyanins produced by
the parent culture after 24 selections [89].
Cell selection and somatic cloning provide useful methods for recovering cells that
produce increased levels of secondary metabolites. However, the lack of rapid screening
methods often impedes application of the method. Deus and Zenk [15] pointed out that
a fluorescence assay could be used to select cells yielding ajmalicine and other major
heteroyohimbine alkaloids from C. roseus cultures. The method was dearly more viable
than the use of radioimmunoassay which can be time-consuming and costly. Indeed, the
technique of cell selection, based on somatic cloning is especially useful when coloured
products can serve as visual selection cues.
Addition of precursors. It has been possible to increase the biosynthesis of specific
secondary metabolites by feeding precursors to cell cultures. For example, amino acids
have been added to cell suspension culture media for production of tropane alkaloids,
indole alkaloids and other products. It is likely that the precursors may be either
incorporated directly into the product, or precursors may enter a specific product indirectly
through degradative metabolism and entry into interrelated pathways. Phenylalanine is a
precursor of rosmarinic acid [23]; addition of phenylalanine to Salvia officialis suspension
cultures stimulated the production of rosmarinic acid and decreased the production time
as well. Pbenylalanine is also the precursor of the N-benzoylphenylisoserine side chain of
taxol; supplementation of Taxus cuspidata cultures with phenylalanine resulted in increased
yields of taxol [27,28]. The literature is replete with examples of the effects of precursor
feeding on the production of secondary metabolites by cultured cells [18]. The evidence
clearly indicates that the timing of precursor addition is critical for an optimum effect. The
effects of feedback inhibition must surely be considered when adding products of a
metabolic pathway to cultured cells.
432 F. DICOSMO and M. MISAWA
BIOTRANSFORMATIONS
Often, plant cells will biotransform a suitable substrate to a more desirable product.
Endress et aL [25] found Rauwolfia serpentina to yield a new indole alkaloid, 6-
hydroxytaumacline, in good yield when the cells were grown in the presence of ajmalicine.
Arbutin, a skin depigmentation agent, is produced by biotransformation of hydroquinone
using C. roseus cells [91]. Addition of the precursor into the liquid culture medium of C.
roseus yields arbutin.
Dombrowski and Alfermann [21] observed the glycosylation of salicylic acid and its
derivatives. They found that cultured Salb¢ matsudana cells glucosylated salicylic acid to
2-O-salicylic acid-13-D-glucoside. The cells also converted salicyl alcohol to salicin (2-0-
salicyl alcohol- 13-D-glucoside) and isosalicylicin (1-O-salicylalcohol- 13-D-glucoside). Salicylic
aldehyde was converted to the 13-D-glucosides of salicylic acid and salicyl alcohol.
Biotransformation of 13-methyldigitoxin to 13-methyldigoxin using D. lanata cells has
been studied extensively by Alfermann (see Table 1). About 600-700 mg of 13-
methyldigoxin per litre was obtained using a 200 L reactor; the process was evaluated for
commercialization by Boehringer Mannheim Company.
Allelix Inc. in Canada [56] established a processes for production of the antitumor
drug, vinblastine, from catharanthine and vindoline using biotransformation, as well as a
simple chemical synthesis. The process is currently being developed for commercialization
by Mitsui Petrochemical in Japan [31]. It is believed that biotransformation processes
including addition of substrates into cultures of suitable cell lines represents one of the
most commercially realistic approaches using plant tissue cultures for product synthesis.
However, the availability of expensive precursors is a key issue and limits economic
viability in some cases.
IMMOBILIZED CELLS FOR SECONDARY METABOLITE PRODUCTION
Compared with plant cell suspension cultures, it is widely held that adherent plant cells
(i.e., immobilized biocatalysts) provide a range of advantages [19,70]. The advantages
include: (1) the extended viability of cells in the stationary (and producing) stage, enabling
maintenance of biomass over a prolonged time period; (2) simplified downstream
processing (if products are secreted); (3) high cell density within relatively small
bioreactors showing reduced costs and risk of contamination; (4) reduced shear stress; (5)
increased product accumulation; (6) flow-through reactors can be used enabling greater
PLANT CELL AND TISSUE CULTURE 433
flow rates; and (7) minimization of fluid viscosity which in cell suspension causes mixing
and aeration problems.
However, the procedures most frequently used for plant cell immobilization, which
are based on entrapment of cells with gels, foams or membranes appear to be either
expensive for large scale application or technically unsound, and consequently none of the
methods has yet been applied commercially for the production of plant derived
biochemicals. The main drawbacks of these methods of immobilization are: (1) gels and
foams are too soft and deformable for use in large scale reactors; (2) membrane systems
are costly; (3) mass transfer is limited and creates undesirable nutrient gradients; (4)
trapped cells are not easily recovered; (5) growing cells tend to rupture the confining
matrix during extended cultivation; and (6) increased hydrodynamic pressures in flow-
through reactors.
In contrast to immobilization by entrapment which has been extensively reviewed
by others [43,69,80], we believe that immobilization by adsorption [19] may represent an
improved approach to cell culture. The advantages are: (1) cultured cells are induced to
adhere to selected polymeric, glass fibre, carbon fibre or ceramic fibre substrates by
controlling the surface tension and electrostatic properties of the liquid medium; (2)
improved mass transfer because no matrix surrounds the cells; (3) improved downstream
processing for excreted products such as proteins and enzymes; (4) immediate reuse of the
media as the cells are totally immobilized, and lower operating costs; (5) the ability of the
cell population to grow to exceedingly high densities with no destruction of the support
(a major advantage as high density cultures usually produce increased levels of
pharmaceuticals); (6) rapid immobilization of large-scale cultures is readily achieved under
physiological conditions; and (7) inexpensive matrices of any geometric configuration can
be used. Furthermore, and possibly fundamentally more important, it seems likely that the
biosynthetic potential of normally slow growing plant cells may be better exploited with
immobilized systems, in terms of both yield and subsequent isolation of the products.
Gel Entrapment Methods
Gel entrapment has been the preferred method of cell immobilization for cultured plant
cells. Calcium alginate gel is the most prevalent gel agent for immobilization. The first
report of immobilization of cultured plant cells described the use of a calcium alginate gel
for the incorporation of spherical clusters of cells of Morinda citrifolia, Digitalis purpurea,
434 F. DICOSMO and M. MISAWA
and Catharanthus roseus [12]. Cell viability was maintained for a 22 day ctilture period in
an appropriate nutrient medium. Calcium alginate entrapped cells are usually prepared
by suspending the cells in a solution of sodium alginate which is subsequently extruded
through an appropriate small diameter opening. The resulting beads 'gel' on contact with
a solution of (50-100 I~M) calcium chloride. Cell distribution within the bead is more or
less homogeneous. The entrapped or immobilized cells can be recovered by chelation of
the calcium ion using EDTA or polyphosphates [53].
The effects of different gel immobilization agents for cells of C. roseus was
evaluated by Brodelius and Nilsson [13]. Cell viability was poor when in the presence of
acrylamide and glutaraldehyde, alginate and carrageenin were non-detrimental and the
best results, vis-a-vis growth and yield of alkaloids were reported for calcium alginate.
Continued growth of cells in the beads ultimately disrupts the gel and free cells emerge.
Consequently, gel entrapment is perhaps most useful with non-dividing cells in a nutrient-
or hormone-limited liquid medium [66].
Surface Immobilization
Surface immobilization takes advantage of the propensity of cultured plant cells to adhere
to inert surfaces immersed in the liquid. The attachment of plant cells to glass culture
vessel surfaces is a feature common to cell suspension cultures and complicates process
control. Recently, several groups have exploited 'surface immobilization' of plant cells
[2,46]. DiCosmo et al. [19] provide a review of plant cell adsorption to surfaces and
immobilization on glass fibres.
The surface immobilization of Catharanthus roseus, Nicotiana tabacum and G&cine
max cultured cells has also been reported [1-3]. A porous ceramic matrix retained cells
effectively. Also a rigid, but porous material of acrylic or rayon fibres bound by phenolic
resin, and a series of non-woven polyester or polypropylene textile materials were effective
immobilization substrates. Archambault et al. [2] suggested that the surface immobilization
of cultured plant cells is advantageous to gel entrapment methods. The surface
immobilization method is simple and gentle; the matrix is inexpensive and retains the
growing biomass efficiently and establishes a well-separated, two-phase system. The
polyester material has been incorporated into rolled column fitted within a laboratory-scale
bioreactors containing C. roseus cells [3].
PLANT CELL AND TISSUE CULTURE 435
DiCosmo et al. [19] discussed the process of surface immobilization of plant cells.
Theoretical considerations as well as some practical examples highlighting the use of glass
fibre mats as the immobilization matrix were provided. The use of glass fibre mats for cell
immobilization was tested in a 5 L bioreactor. The production of alkaloids by C. roseus,
and berberine and columbamine by Thalictrum rugosum cells immobilized on mats was
examined. Immobilization was found to be relatively rapid and occurred efficiently under
physiological conditions. The immobilization was firm and irreversible, and the system was
maintained for an extended period. The accumulation of indole alkaloids and tryptamine,
by glass fibre-immobilized cells of C. roseus was lower than in freely suspended cells. In
contrast, the accumulation of berberine, by immobilized and suspension cultured cells of
T. ntgosum was similar. The growth rate of immobilized cells of C. roseus and T. ntgosum
was lower than freely suspended cells. The increase in the accumulation of indole alkaloids
(Table 3) by cells of C. roseus when entrapped in alginate beads may arise as a response
to phosphate limitation, rather than due to the immobilization in alginate beads. Glass
fibre-immobilized C. roseus cells yield decreased production of indole alkaloids; this is in
accord with other non-alginate immobilized systems.
The process of cell immobilization by adsorption to the glass fibre mat is a
generally applicable phenomenon. The process involves non-specific, thermodynamic and
electrostatic interactions, as well as passive entrapment. The immobilization demonstrates
the industrial potential of the system, as well as being a technique of evaluating the
physiology and metabolism of adherent plant cells free of the constraints of an
encapsulating gel.
Other Approaches
The regulation of plant secondary metabolism at the biochemical and genetic levels will
undoubtedly lead to improved production systems in the near future [19a], particularly for
phenylpropanoid-derived substances. Selection of variant cell lines with increased
biosynthetic abilities for secondary metabolites will also provide improvements to cell
culture technology [8a]. These topics have been detailed authoritatively elsewhere [8a] and
will not be discussed here.
436 F. DICOSMO and M. MISAWA
Table 3. Reported effect of various immobilization strategies on the accumulation of indole alkaloids by cultured cells of Catharanthus roseus.
Immobilization Product Product accumulation Reference system relative to suspensions
Alginate Ajmalicine (+)* Brodelius eta/- [8] Alginate Tryptamine ( - )* Maierus and Pare~ux I531
Ajmalicine Serpentine
Alginate Ajmalicine (+) Asada and Shuler [1] Agar/carrageenin Ajmalicine (-) Brodelius et at [8] Dialysis tubing Total alkaloids (-) Payne ct al. [63] Non-woven polyester Strictosidine lactam (-) Archambault eta/. [3]
Ajmalicine Tabersonine Serpentine
Glass fibres Tryptamine (-) DiCosmo et a/- [19] Catharanthine Ajmalicine
* (+) = increase; (-) = decrease
EXAMPLES OF SECONDARY METABOLITES AS CELL CULTURE PRODUCTS
A variety of plant derived alkaloids are used as pharmaceuticals. The typical tropane
alkaloids, atropine, hyoscyamine, scopolamine and cocaine, are widely used as antagonists
of the parasympathetic nervous system. Research on cell culture production of these
compounds has been active for more than 25 years. Industrial production has yet to
succeed because of the low yield from cultured cells. Nevertheless, the bisindole alkaloid
vinblastine, will likely be produced commercially by Mitsui Petrochemical in Japan using
a combination of plant cell culture and chemical synthesis.
Morphinan Alkaloids
Codeine is an analgesic and cough-suppressant from Papaver somni f emm, that is also the
traditional commercial source of morphine which can be converted to codeine. Mature
capsules of P. bracteatum also accumulate up to 3.5% thebaine which is convertible to
PLANT CELL AND TISSUE CULTURE 437
codeine. Production of codeine by undifferentiated cells ofPapaver spp. has met with little
success. Kamimura et al. [45] reviewed alkaloid production and indicated that
morphogenetic differentiation of cultured cells of P. bracteamm was required for
stimulating thebaine biosynthesis. Other researchers have confirmed similar findings with
P. bracteamm and P. somniferum [75,76].
The efficient production of thebaine and codeine using cell culture systems by de
novo synthesis has not been successful; however, the biotransformation of codeinone to
codeine with immobilized cells of P. somnifen~m has been shown to be possible [33]. The
conversion yield was 70.4%, and about 88% of the codeine converted was excreted into
the medium. Eilert et al. [22] showed that fungal mycelium (elicitor) ofBottytis sp. induced
production of sanguinarine by cultured P. sornnifentm cells. The presence of the elicitor
increased alkaloid production 26-fold in comparison with the elicitor-free culture.
Berberine
Berberine is an isoquinoline alkaloid which is found in roots of Coptis japonica and the
cortex of Phellondendron amurense. Berberine chloride is used for intestinal disorders in
the Orient. Five to six years are required to produce Coptis roots as the raw material.
Furuya et aL [34] investigated the production of berberine by Coptisjaponica cell cultures
while Yamada and Sato [88] at Kyoto University selected a high berberine producing cell
line of C. japonica. The latter cell line was subsequently transferred to Mitsui
Petrochemical where the yield of berberine was further improved. Hara et al. [39]
determined that addition of 10 -8 M gibberellic acid into the medium stimulated berberine
accumulation to 1.66 g'L -1 of medium. By careful selection several high yielding cell lines
were isolated. The Mitsui group produces berberine at a large scale with a productivity of
1.4 g.L -1 over 2 weeks. A high-density cell culture process for producing berberine more
efficiently has been developed at Mitsui. Addition of spermidine to Thalictrum mbzus is
known to stimulate the production of berberine in suspension culture [38]. Other
polyamines such as cadaverine, putrescine and spermine are ineffective [38]. Maximum
yield of berberine was obtained in the presence of 2 mM spermidine.
Tropane Alkaloids
Studies on the production of tropane alkaloids by plant tissue cultures have been ongoing
since the discovery of tropanes in Atropa belladonna callus tissue. However, the
438 F. DICOSMO and M. MISAWA
concentrations of scopolamine and hyoscyamine in cultured cells are generally low and
plant cell culture technology has not yet enabled commercial production of these alkaloids.
Atropine, scopolamine and hyscyamine have been produced by cultured roots of Atropa
and Dubosia [30].
Cardenolides
Cardiac glycosides or cardenolides are derived commercially from Digitalis species. Some
cardenolides are used in the treatment of heart diseases. Cultivation of Digitalis plants in
fields of several countries, including the Netherlands, Hungary and Argentina yields the
commercial quantity of clinical drugs. Lanoxin is the Burroughs Wellcome digoxin product
that has major markets in the United States and Italy; total sales being about 6000 kg per
year with a market value of US$50 million. Other producers of cardenolides are
Boehringer Mannheim, Merck Darmstadt and Beiersdorf AG in Germany.
There are many studies concerning the production of cardiac glycosides by Digitalis
tissue cultures [66]. Generally, the yield of product is very low and decreases during
successive culture transfers. Many researchers have concluded that morphological
differentiation causes an increase in productivity of cultured cells. For example, Lui and
Staba [51] showed that organ cultures ofD. lanata leaves and roots produced cardenolides;
the amount of digoxin in the tissues increased with age [52]. Hirotani and Furuya [41]
found that differentiation of callus tissues of D. purpurea led to formation of cardinolides.
Hagimori et al. [37] of Japan Tobacco Inc. cultivated shoot-forming tissues of D, purpurea
in a 3 L jar fermenter and detected high concentrations of cardiac glycosides, including
digitoxin. The culture of differentiated tissue is necessary for secondary metabolites
production in some cases. Secondary metabolites such as digitoxin and digoxin have been
found in cell tissues cultures of D. lanata and D. purpurea. Other such compounds include
cholesterol, campesterol, stigmasterol, [l-sitosterol and 4-hydroxy-digitolutein. As might be
expected, the production of such products decrease with the total length of time the cells
have been in culture [47].
Biotransformation reactions using Digitalis plant cells appear to present a viable
commercial process. D. lanata and D. purpurea callus cultures have been shown to rapidly
yield pregnane from progesterone [35]. Organ cultures (leaf and root) of D. lanata and
shoot-forming callus tissues of D. purpurea produced increased amounts of digoxin and/or
digitoxin when progesterone was an adjuvant in the culture medium [37,52]. Indeed, the
PLANT CELL AND TISSUE CULTURE 439
biotransformation of digitoxin to digoxin iasing D. lanata cells provides a commercially
interesting approach to the production of digoxin. Digitalis leaves contain a relatively large
amount of digitoxin used as a substrate in the biotransformation. The biotransformation
is a 12 I~-hydroxylation reaction of digitoxin. The 13-methyldigitoxin has been found to be
the best substrate in the biotransformation since methyldigoxin is the major product.
Immobilized cells of D. lanata have been employed in semi-continuous culture. The results
of a typical biotransformation after 17 days in a 20 liter bioreactor are shown in Table 4.
The process was tested in large scale reactors by Boehringer Mannheim Company in
Germany; however, a commercial operation has not been attempted.
Table 4. Biotransformation of 13-methyldigitoxin to 13-methyldigoxin by Digitalis lanata cells in a 20 L reactor.
13-Methyldigitoxin added 17.24 g (100%) Unconverted 13-methyldigitoxin 2.04 g (11.8%) 13-Methyldigoxin formed 14.36 g (81.7%) By-product 0.28 g (1.4%) Yield 94.90%
L-DOPA
L-3,4-dihydroxyphenylalanine (L-DOPA) is an important intermediate in plant metabolism
and is a precursor of alkaloids, betalain, melanin, and other metabolites. It is used as a
potent drug in the treatment of Parkinson's disease. Callus tissue of Mucana pruriens can
accumulate 25 mg.L -1 DOPA, in medium containing a relatively high concentration of
2,4-D [11]. Cells of M. pruriens immobilized within alginate beads produced DOPA from
tyrosine in yields of up to 2% of the dry cell weight and the product was secreted into the
medium. Teramoto and Komamine [81] used callus tissues of Stizolobium hassjoo (Mucuna
hassjoo), M. pntriens and M. deeringiana, to study L-DOPA production. The highest yield
(80 ismol.g -1 fresh weight) was obtained when S. hassjoo cells were cultivated in MS
medium containing 0.025 mg.L -1 2,4-D and 10 mg.L -1 kinetin.
440 F. DICOSMO and M. MISAWA
Valepotriates
Plants in the Valerianaceae genus have been used extensively as folk medicines [8]. For
example, Nardostachys jatamansi, Valeriana wallichii and F. officinalis L var. angustifolia
have been used in India and N. chbzensis has been employed in China for hundreds of
years. Partrinia sp. are also being used as sedatives in the former Soviet Union. Although
the active principles in these plants have not been identified, a group of compounds with
sedative, tranquillizer, and cytotoxic properties have been termed 'valepotriates.'
Callus tissues of nine different species of Valerianaceae were studied. Fedia
cornucopiae and Valeriana locusta cells yielded more valepotriates than found in the intact
plants. L-leucine was considered as a precursor of the valepotriates; hence, Baker and
Chavadej [8] isolated cell lines of F. wallichii resistant to trifluoroleucine, a leucine analog.
However no increase in the production of valepotriates was noted. One strain of F.
wallichii resistant to nystatin yielded 88 mg.g -1 (dry weight) valepotriates. A suspension
culture of F. wallichii treated with colchicine, which was expected to induce polyploid cells
yielded higher amount valepotriates than untreated cultures [8]. A two-phase culture,
developed by addition of RP-8 (Merck) into the culture medium induced secretion of
valepotriates into the medium thereby increasing the total yield of valepotriates. Certain
plant bioregulators, such as dimethyl-morpholinium-bromide, dimethyl-piperidinium-
bromide, dimethyl-piperidinium-chloride as well as 2-(3,4-dichloro-phenoxy)-triethylamine
added to cultures ofF. comucopiae and E wallichff at concentrations of 0.01 to 0.04 mmol,
during the early exponential growth stages of the cells, induced valepotriate accumulation.
Antitumor Compounds
Plants are an attractive source of novel antitumor compounds. A recent example being
taxol. The National Cancer Institute in the United States, for example, has conducted
extensive screening of plants since 1955 and has identified various potent compounds from
these [77] . These antitumor compounds include maytansine, tripdiolide,
homoharringtonine, bruceantin, ellipticine, thalicarpine, indicine-N-oxide, and baccharin.
In addition, other higher plant products including vinblastine, vincristine, the
podophyllotoxin derivative etoposide and camptotbecin and its derivative have already
been marketed as very important anticancer drugs. Taxol from Taxus brevifolia and related
species is now used in treating ovarian and breast cancer and is in clinical trials for other
neoplasms. Generally, plants produce relatively low amounts of secondary metabolites
PLANT CELL AND TISSUE CULTURE 441
showing antitumor activity (Table 5). An alternative to whole plant extraction of plant
natural products is through plant cell culture [57,58]. In the following we cite examples
were plant cell cultures have been used to study the possible production of antitumor
agents.
Table 5. Antitumor compounds isolated from higher plants [58].
Antitumor compounds Yield (% of plant dry weight)
Baccharin 2.0 x 10 -2 Bruceantin 1.0 x 10 -2 Camptothecin 5.0 x 10 -3 Ellipticine 3.2 x 10 -5 Homoharringtonine 1.8 x 10 -5 Maytansine 2.0 x 10 -5 Podophyllotoxin 6.4 x 10 -1 Taxol 5.0 x 10 -1 Tripdiolide 1.0 x 10 -3 Vinblastine, vincristine 5.0 x 10 -3
Camptotheein. Camptotheca acumb~ata, a plant native of North China, produces a potent
antitumor alkaloid, camptothecin. It is highly active in Walker rat carcinosarcoma and
mouse leukemia, p388 and L1210; clinical trials in patients with gastrointestinal cancer
demonstrated toxicity. Sakato and Misawa [71] induced callus from the stem of C.
acum#zata on MS solid medium containing 0.2 mg.L -1 2,4-D and 1 mg.L -1 kinetin and
developed liquid cultures in the presence of gibberellin, L-tryptophan and conditioned
medium. After 15 days in liquid suspension, cells yielded 0.0025% on a dry weight basis
camptothecin, i.e. 1/20 the amount produced by the intact plant. A.J. van Hengel et aL [84]
found 0.998 mg camptothecin per liter of medium; the compound was accumulated in C.
acumbzata cells cultivated in MS medium containing 4 mg-L -1 NAA. 10-
Hydroxycamptothecin, that is less toxic than camptothecin is a promising derivative and
is in clinical trials in the United States.
Homoharringtonine. Homoharringtonine, harringtonine and isoharringtonine, are derived
from Cephalotaxus harringonia [64]. These alkaloids are complex esters of the inactive
alcohol, cephalotaxine, and inhibit the growth of several neoplasms. Delfel and Smith [14]
442 F. DICOSMO and M. MISAWA
found about 5-10 mg of cephalotaxine related compounds per kg dry wt. of callus tissues
grown for 3 to 6 months; these levels were approximately 1 to 3% of the amounts found
in the intact plant.
MS medium containing 1 mg.L - t kinetin and 3 mg.L -1 NAA can be used to
induce the callus from C. harringtonia [57,58]; radioimmunoassay showed that the levels
of cephalotaxine and its esters were approximately 1/300 of the intact plant.
Podophyllotoxin. Podophyllum peltatum, common to eastern North America contains the
antitumor lignan, podophyllotoxin. It is active against KB cells and certain viral diseases
and skin cancer [62]. A semi-synthetic derivative of podophyllotoxin, etoposide, is active
against brain tumor, lymphosarcoma and Hodgkins' disease and was approved by the US
Food and Drug Adminstration; Bristol-Myers Squibb is among the largest manufacturers
of the drug.
Podophyllotoxin accumulation by P. peltatum cell cultures was investigated initially
by Kadkade [44], who found that a combination of 2, 4-D and kinetin in the medium
supported the highest amount of its production. Red light stimulated production of the
compound in cell culture systems. Woerdenberg et al. [87] used 13-cyclodextin entrapped
coniferyl alcohol as a precursor for podophyllotoxin production in Podophyllum hexandrum
cell suspension cultures. Addition of 3 mM coniferyl alcohol yielded 0.013% on a dry
weight basis podophyllotoxin accumulation in cells; however, cells not provided the
precursor yielded only 0.003%. Confierin was a better precursor in stimulating the yield
(0.055%) of the compound. Cell suspension cultures of Callitris drummondii were also
reported to accumulate podophyllotoxin-l~-D-glucose. The cells produced approximately
0.02% (dry weight basis) podophyllotoxin in the dark, and 85-90% of the lignans extracted
were [3-D-glucosides; in the light, however, the yield of podophyllotoxin-l~-D-glucose
increased to 0.11%.
Smollny et al. [74] reported that callus tissues and suspension culture cells of Lilium
album produced podophyllotoxin. One of the cell lines produced 0.3% podophyllotoxin,
and lower amounts of 5-methylpodophyllotoxin, lariciresinol and pinoresinol after 3 weeks
of cultivation. Callus tissue of P. hexandrum was reported by Heyenga et al. [40] to
produce podophyllotoxin, 4'-demethyl-podophyllotoxin and podophyllotoxin-4-O-glucoside
when the callus was incubated in B5 medium containing 2, 4-D, gibberellic acid and 6-
PLANT CELL AND TISSUE CULTURE 443
benzylaminopurine. The levels of podophyllotoxin and its derivatives were similar to those
found in the intact plant from which the callus was induced.
Vinblastine and vincristine. The indolic alkaloids, vinblastine and vincristine are used in
cancer chemotherapy for treating various leukemias, Hodgkin's disease and solid tumors.
The drugs are produced commercially by extraction of large quantities of Catharanthus
roseus plant material. However, the intact plant, contains low concentrations of drugs
(0.0005% dry weight basis). As an alternative to whole plant extraction, plant cell cultures
have been employed in efforts to produce vinblastine and vincristine. The literature in this
area is voluminous. There are reports of vinblastine and vincristine being produced in cell
culture or organ culture, but the reports cite very low levels of compound, or the report
needs verification. There are no reports of vinblastine and vincristine accumulation in long
term plant cell suspension cultures, nor has the accumulation of vindoline been
demonstrated authoritatively.
Misawa and his colleagues at Allelix Inc. in Canada [56] studied the production of
vinblastine and established an economically viable process based on production of
catharanthine by plant cell systems and a simple chemical or an enzymatic coupling of
catharanthine with vindoline extracted from the intact plant.
Vinblastine is composed of catharanthine and vindoline; the plant produces much
more vindoline (0.2%) than catharanthine, and vindoline is less expensive than
catharanthine. Catharanthine production in high yield by selected C. roseus cell lines
derived from anther tissue has been demonstrated [31]. For example, cells are grown in
MS liquid medium supplemented with 3% sucrose, 1 mg.L -1 NAA and 0.1 mg.L -1
kinetin under continuous diffuse light. The results of the experiments showed that MS
medium was beneficial for catharanthine production; however, different amounts of
hormones were required for each cell line to achieve optimum results. Addition of various
compounds to the medium stimulated the production of alkaloids. Vanadyl sulphate,
abscisic acid and sodium chloride showed significant effects on the production of
catharanthine [73]. Subsequently, the Allelix group [24] tried to couple enzymatically, and
chemically, the catharanthine produced by the cell culture process with commercially
available vindoline. A crude preparation of 70% ammonium sulphate precipitated protein
from the cultured cells of C. roselts was used as an enzyme source. The reaction mixture
contained catharanthine, vindoline, Tris buffer, pH 7.0 and the crude enzyme; the mixture
444 F. DICOSMO and M. MISAWA
was incubated at 30°C and for 3 hours. The products of the reaction were various dimeric
alkaloids including vinamidine, 3-(R)-hydroxyvinamidine and 3',4'-anhydrovinblastine. The
oxidized derivatives of anhydrovinblastine, leurosine and catharine were detected during
the early stages of the reaction. Manganese (II) chloride and either FAD or FMN
stimulated the coupling, but neither vinblastine nor vincristine was detected in the mixture.
However, a substantial amount of anhydrovinblastine was formed as the major reaction
product in the presence of excess sodium borohydride, added to the mixture after
incubation. The protein fraction with dimerizing activity was partially purified using gel
filtration and isoelectric focusing; five isozymes were resolved by Endo et al. [24]. All of
the fractions obtained had peroxidase activity. With the partially purified protein extracts
Endo et al. [24] showed that anhydrovinblastine was formed in approximately 50% yield.
It was found by the Allelix group that ferric ion catalyzes the dimerizing of catharanthine
and vindoline in the absence of the enzyme, and the products of the reaction were
anhydrovinblastine and vinblastine in 52.8% and 12.3% yield, respectively.
This relatively efficient process for producing vinblastine is likely to be commercially
viable. The technology was transferred from Allelix to Mitsui Petrochemicals Industry of
Japan for further development. Subsequently, the Mitsui group used high-cell density
cultures and improved further the yields of catharanthine to 230 mg.L -1 per week [31].
The yield of vinblastine via chemical coupling was also improved; the yield of vinblastine
from anhydrovinblastine was increased to 50% in the presence of ferric chloride, oxalate,
maleate and sodium borohydride.
Bede and DiCosmo [6,7] have also investigated the production of
anhydrovinblastine. A two-enzyme system, contained glucose oxidase and horseradish
peroxidase for sequential production of I-I20 2 and anhydrovinblastine, from glucose, and
catharanthine and vindoline, respectively. Peroxidase(s) require hydrogen peroxide for
dimerizing activity, but with excess H20 2 the reaction may be inhibited. Glucose oxidase
was used for the controlled, continuous production of H202 at relatively low but effective
levels, thus minimizing oxidative reactions. The yield of anhydrovinblastine in the presence
of various peroxidase enzymes is presented in Table 6. The pure enzymes were
immobilized on Eupergit C beads, and the system was shown to catalyze the synthesis of
anhydrovinblastine.
PLANT CELL AND TISSUE CULTURE 445
Table 6. Comparison of the ability of different peroxidase preparations to catalyze the formation of anhydrovinblastine [6].
Mean Concentration of Alkaloids Yield Peroxidase Activity (± standard deviation)
(U/assay) Catharanthine Vindoline AVLB AVLB [llmol] ll~moll [~tmol] (%)
HrP I 10.4 0.27 0.12 0.44 54.7 (± 0.03) (± 0.01) (± 0.07)
HrP VI 11.36 0.37 0.17 0.4 50.2 (-+ 0.01) (± 0.01) (-+ 0.01)
HrP VII 11.32 0.44 0.25 0.36 44.6 (± 0.01) (± 0.01) (_+ 0.02)
HrP IX 13.01 0.51 0.26 0.23 19.2 (_+ 0.03) (± 0.01) (± 0.03)
HrP XI 0 1.04 0.51 0 0 (± 0.20) (± 0.04)
HrP XII 11.04 0.68 0.36 0.14 17.8 (_ 0.03) (_+ 0.01) (± 0.02)
Lactoperoxidase 8.82 1.03 0.57 0 0 (± 0.12) (± 0.03)
Control 1.75 0.80 0 (_+ 0.07) (_+ 0.02)
The reaction mixture contained: Catharanthine (0.70 mM), vindoline (0.32 mM), GO (0.12 mg.mL -1 (1.0 U)), peroxidase preparation (approximately 11.0 U) and glucose (4.4 mM) were incubated in 2.5 mL of 0.1 M MES buffer, pH 6.8 for 45 minutes at 30°C. Peroxidase activity was calculated from spectrophotometric measurements of guaiacol oxidation. Final concentrations represent the mean of a triplicate experiment ___ the standard deviation. Control experiment was conducted in the absence of enzymes.
Paclitaxel. Under the intensive National Cancer Institute screening program of antitumor
compounds in the United States, Wall isolated a biologically active product from the bark
of Taxus brevifolia in 1965; the compound was active against KB cells and in 1969 pure
taxol was isolated and its chemical structure was elucidated in 1971 [85]. The diterpene
amide paclitaxel (Taxol ®) has shown activity against B16 mouse melanoma tumor, the
MX-1 human mammary xenograft and CX-1 colon xenografts. The mechanism action of
taxol is unique; it promotes microtubule polymerization. Taxol ® is now a trademark of
Bristol-Myers Squibb and is approved for the treatment of ovarian and breast cancer. The
chemistry and biology of paclitaxel have been reviewed recently [61].
446 F. DICOSMO and M. MISAWA
The US Food and Drug Adminstration approved paclitaxel at the end of 1992.
Bristol-Myers Squibb produces the drug for use in the treatment of refractory ovarian
cancer; it is now being manufactured by extraction from the bark of wild-grown T.
brevifolia and needles of other Taxus spp. A semisynthetic method is also available for
paclitaxel production. The demand for paclitaxel is increasing and undoubtedly it will be
used for treating other neoplasms.
Plant tissue and cell culture technology, including biotransformation processes from
baccatin and related taxoids extracted from leaves of Taxus spp. [36] may lead to improved
production of paclitaxel. Cell culture methods for Taxus cuspidata and T. canadensis were
developed by DiCosmo's group [26-29] and others [78]. The cell cultures yielded taxol and
related taxanes. Subsequently, the group improved the growth of T. cuspidata cell cultures,
as well as improving the production of taxol by feeding phenylalanine to selected cell lines.
The kinetics of paclitaxel accumulation indicated that its appearance in the media of
suspension cultures had two peaks. The first, appeared in the early phase of the growth
cycle, and the second flush of paclitaxel appeared in the late stage of the growth cycle.
Further improvement to the production of paclitaxel was brought about by feeding cell
suspension cultures benzoic acid, N-benzoylglycine, serine and glycine. Indeed, there is
good evidence that paclitaxel and related taxoid production in Taxus cuspidata cell cultures
can be improved to industrially interesting levels.
Two US companies, ESCA genetics and Phyton Catalytic have suggested that
paclitaxel will be produced by commercially using proprietary cell culture technology.
However, details of the processes have not been disclosed; nonetheless, the production of
paclitaxel by cell culture methods on a commercial scale remains speculative. Japanese
industries, such as Nippon Steel Corp., Nippon Oil Company and Mitsui Petrochemical
Industry have investigated paclitaxel production using cell culture methods. For example,
Saito et al. [70a] of Nippon Steel reported a yield of 0.05% of paclitaxel (dry weight basis)
in T. brevifolia cultured cells. Tabata et aL [78a] of Mitsui Petrochemical has described the
production of 35 mg.L -1 paclitaxel, 18 mg.L -1 baccatin III, and 18 mg'L -1
cephalomannine simultaneously from suspension cultured T. baccata cells after 21 days of
cultivation.
Although the use of plant cell culture technology for the production of valuable
plant products has yet to be realized, we believe that success will occur as the
PLANT CELL AND TISSUE CULTURE 447
understanding of the metabolism of plant cells in culture improves, with concomitant
improvements to plant cell culture fermentation technology.
2.
3.
4.
5.
6.
7.
8.
8a.
9.
10.
11.
12.
13.
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