BIOTECHNOLOGY APPROACHES FOR IN VITRO PRODUCTION OF FLAVONOIDS
Alia Amer
Address(es):
Medicinal & Aromatic Dep., Horticulture Research Institute, Agricultural research Center, Cairo, Egypt.
*Corresponding author: dr_aliaamer@yahoo.com
doi: 10.15414/jmbfs.2018.7.5.457-468
ARTICLE INFO
ABSTRACT
Received 5. 10. 2017
Revised 13. 12. 2017
Accepted 5. 2. 2018
Published 1. 4. 2018
Flavonoids are small molecular secondary metabolites synthesized by plants with various biological activities such as antiinflammatory, anti-carcinogenic, antioxidant, etc. Flavonoids occur naturally in fruits, vegetables, medicinal plants and beverages such
as tea and wine. Biotechnology offers different in vitro systems which have been developed to exploit these active ingredients such as,
in callus cultures, cell suspension cultures which are the emerging fields of biotechnology to investigate and enhance the production of
these products. Along with this, hairy root culture and transformation techniques have been studied widely for flavonoid production.
Nano-treatment is a novel way for improvement of flavonoids production. the present review focus on describing the flavonoids
biochemistry, regulation of biosynthesis, as well as the Biotechnology and Nano-biotechnology tools for in vitro production of
flavonoids.
Regular article
Keywords: Flavonoid, Biosynthesis, Medicinal Plants, In Vitro Production, Nanoparticles Applications
INTRODUCTION
Plants are essential for life as they supply all animals on the earth, including
humans, with essential foods. Plants are being the main source of
pharmacologically active compounds, with many blockbuster drugs being
derived directly or indirectly from plants. Despite the current dependence on
synthetic chemistry to develop and manufacture drugs, yet the contribution of
plants to disease treatment and prevention is still enormous. However, several
challenges have been associated with the supply of biologically active
pharmaceuticals from natural sources. Alternative avenues for plant products
have gained importance during the past few years among which plant
biotechnology has a key role to play in plant based industries (Veeresham and
Chitti, 2013).
Plant in vitro techniques becomes an important part of biotechnological tool that
offers a great potential solution for the propagation of endangered and superior
genotypes of medicinal plants, which could be released to their natural habitat or
cultivated on a large scale for the pharmaceutical product of interest. The
enhanced production of secondary metabolites from plant cell cultures through
elicitation has opened up a new spot of research which could have important
economic benefits for pharmaceutical industry (Devi et al., 2008).
Flavonoids are found in most terrestrial vascular plants, which belong to a group
of natural phenolic substances with variable chemical structures. They are found
in fruits, vegetables, grains, tree barks, roots, stems, flowers, as well as tea and
wine (Hermann, 1976; Stafford, 1991; Harborne and Williams, 2000). More
than 6000 different flavonoids have been identified, many of which are
responsible of the attractive colours of flowers, fruits and leaves (Nijveldt et al.,
2001).
The interesting biological activities of flavonoids have prompted the intensive
research on the physiological properties of these compounds as well as their
effects on human health (Rusak et al., 2002). This review is entended to compile
the most relevant research on flavonoids to though light on progress in using
current various techniques in producing flavonoids and the need to consider more
effective research methods with emphathis on nanotechnology in this context.
FLAVONOIDS
(Stafford, 1990). Flavonoids are aromatic secondary plant metabolites, which
have been recognized as important due to their physiological (Buslig and
Manthey, 2002; Forkmann, 1992; Cody et al., 1988) and pharmacological (Di
Carlo et al., 1999; Wang, 1999; Tapiero et al., 2002; Manach and Donovan,
2004; Sharma, 2006; Cermak and Wolffram, 2006; Ortuno et al., 2006) role
and their health benefits (Valenzuela et al., 2003; Hooper and Cassidy, 2006).
Marinova et al. (2005) demonstrated that the phenolics are ubiquitous secondary
metabolites in plants, comprising a large group of biologically active ingredients
(above 8000 compounds) from simple phenol molecules to polymeric structures
with molecular mass above 30000 Da. Based on the number of phenol subunits,
the modern classification forms two basic groups of phenolics, simple phenols
and poly phenols. The group of simple phenols contains carboxyl group
underlying the specificity of their function. Polyphenols contain at least two
phenol rings, where Flavonoids belong to this group which are a subject of
comprehensive studies in recent years. More than 4000 flavonoids have been
identified in different higher and lower plant species. The classification of
polyphenols presents a challenge, as some classes such as chalcones, flavanones,
and flavan-3-ols are both intermediates as wells as end products accumulating in
the plant biosynthesis process, while other classes such as flavones and flavonols
are identified as end products in the biosynthesis (Andrae-Marobela et al.,
2013).
Available reports tend to show that secondary metabolites of phenolic nature,
including flavonoids are responsible for the variety of pharmacological activities
(Mahomoodally et al., 2005; Pandey, 2007). Flavonoids are hydroxylated
phenolic substances and are known to be synthesized by plants in response to
microbial infection (Dixon et al., 1983). Their activities are structure dependent
as the chemical nature of flavonoids depends on their structural class, degree of
hydroxylation, other substitutions and conjugations, and degree of polymerization
(Kelly et al., 2002). Flavonoids also act as a secondary antioxidant defence
system in plant tissues exposed to different abiotic and biotic stresses. Flavonoids
are located in the nucleus of mesophyll cells and within centres of reactive
oxygen species (ROS) generation. They also regulate growth factors in plants
such as auxin (Agati et al., 2012). Biosynthetic genes have been assembled in
several bacteria and fungi for enhanced production of flavonoids (Du et al.,
2011). In order to better understand the role and mechanism of flavonoids, their
chemistry and biosynthesis seems proper to be presented.
Plant flavonoids are a large group of very different compounds sharing the
common feature of phenol moieties (Harborne and Williams, 2000;
Grotewold, 2006). They are, with a few notable exceptions, plant metabolites
deriving from the shikimate pathway and the phenylpropanoid metabolism
457
J Microbiol Biotech Food Sci / Alia Amer 2018 : 7 (5) 457-468
Flavonoids occur as aglycones, glycosides, and methylated derivatives. The basic
flavonoid structure is aglycone (Figure 1 and Table 1). Six-member ring
condensed with the benzene ring is either a �-pyrone (flavonols and flavanones)
or its dihydro derivative (flavonols and flavanones). The position of the
benzenoid substituent divides the flavonoid class into flavonoids (2-position) and
isoflavonoids (3-position). Flavonols differ from flavanones by hydroxyl group at
the 3-position and a C2–C3 double bond (Narayana et al., 2001). Flavonoids are
often hydroxylated in positions 3, 5, 7, 2, 3', 4', and 5'. Methy l ethers and acetyl
esters of the alcohol group are known to occur in nature. When glycosides are
formed, the glycosidic linkage is normally located in positions 3 or 7 and the
carbohydrate can be L-rhamnose, D-glucose, glucorhamnose, galactose,
orarabinose (Middleton, 1984).
Studies on flavonoids by spectroscopy showed that most flavones and flavonols
exhibit two major absorption bands: Band I (320–385nm) represents the B ring
absorption, while Band II (250–285 nm) corresponds to the A ring absorption.
Functional groups attached to the flavonoid skeleton may cause a shift in
absorption such as from 367nm in kaempferol (3,5,7,4'-hydroxyl groups) to 371
nm in quercetin (3,5,7,3',4'-hydroxyl groups) and to 374 nm in myricetin
(3,5,7,3',4',5'-hydroxyl groups) (Yao et al., 2004). The absence of a 3-hydroxyl
group inflavones distinguishes them from flavonols. Flavanones have a saturated
heterocyclic C ring, with no conjugation between the A and B rings, as
determined by their UV spectral characteristics (Rice-Evans et al., 1996).
Flavanones exhibit a very strong Band II absorption maximum between 270 and
295 nm, namely, 288 nm (naringenin) and 285 nm (taxifolin), and only ashoulder
for Band I at 326 and 327 nm. Band II appears as one peak (270 nm) in
compounds with a mono substituted B ring, but as two peaks or one peak (258
nm) with a shoulder (272 nm) when a di-, tri-, or o-substituted B ring is present.
As anthocyanins show distinctive Band I peak in the 450–560 nm region due to
hydroxyl cinnamoyl system of the Bring and Band II peaks in the 240–280 nm
region due to the benzoyl system of the A ring, the colour of the anthocyanins
varies with the number and position of the hydroxyl groups (Wollenweber and
Dietz, 1981).
FLAVONOIDS CHEMISTRY AND BIOSYNTHESIS
Chemistry
Flavonoids are a group of natural compounds with variable phenolic structures
and are found in plants. In 1930 a new substance was isolated from oranges,
where at that time it was believed to be a member of a new class of vitamins and
designated as vitamin P. Later on, it became clear that, this substance was a
flavonoid (rutin) and till now more than 4000 varieties of flavonoids have been
identified (Middleton, 1998).Chemically flavonoids are based upon a fifteencarbonskeleton consisting of two benzene rings (A and B as shown in Figure 1)
linked via a heterocyclic pyrane ring(C). They can be divided into a variety of
classes such as flavones (e.g., flavone, apigenin, and luteolin), flavonols
(e.g.,quercetin, kaempferol, myricetin, and fisetin), flavanones (e.g., flavanone,
hesperetin, and naringenin), and others.Their general structures are shown in
Table 1. The various classes of flavonoids differ in the level of oxidation and
pattern of substitution of the C ring, while individual compounds within a class
differ in the pattern of substitution of the A and B rings (Middleton, 1998).
Figure 1 Basic flavonoid structure
Table 1 Main flavonoids classes Structure
Groups
Structure backbone
Flavones
Examples
Chrysin
Apigenin
Luteolin
Flavonols
Quercetin
Galangin
Kaempferol
Flavanones
Hesperetin
Naringenin
Flavanonol
Taxifolin
Isoflavones
Genistein
458
J Microbiol Biotech Food Sci / Alia Amer 2018 : 7 (5) 457-468
Flavan-3-ols
Catechin
Epicatechin
Biosynthesis
Regulation of flavonoid biosynthesis
Flavonoids are synthesized through the phenylpropanoid pathway, transforming
phenylalanine into 4-coumaroyl- CoA, which finally enters the flavonoid
biosynthesis pathway (Figure2). The first enzyme specific for the flavonoid
pathway, chalcone synthase, produces chalcone scaffolds from which all
flavonoids derive. Although the central pathway for flavonoid biosynthesis is
conserved in plants, depending on the species, a group of enzymes, such as
isomerases, reductases, hydroxylases, and several Fe2+/2-oxoglutarate-dependent
dioxygenases modify the basic flavonoid skeleton, leading to the different
flavonoid subclasses (Martens et al., 2010). Last, tranferases modify the
flavonoid backbone with sugars, methyl groups and/or acylmoieties, modulating
the physiological activity of the resulting flavonoid by altering their solubility,
reactivity and interaction with cellular targets (Bowles et al., 2005; Ferrer et al.,
2008; Falcone Ferreyra et al., 2012).
Evidence is emerging showing that consecutive enzymes of the phenylpropanoid
and flavonoid biosynthesis are organized into macromolecular complexes that
can be associated with endo membranes (Kutchan, 2005). Metabolic channeling
in plant secondary metabolism enables plants to effectively synthesize specific
natural products and thus avoid metabolic interference. The existence of
cytochrome P450 mono oxygenases (P450s)-related metabolons has been
demonstrated: direct and indirect experimental data describe P450 enzymes in the
phenylpropanoid, flavonoid, cyanogenic glucoside, and other biosynthetic
pathways (Winkel, 2004; Ralston and Yu, 2006). Additional evidence for the
channeling of intermediates between specific isoforms of phenylalanine
ammonialyase and cinnamate -4- hydroxylase has been provided using transgenic
tobacco plants expressing epitope-tagged versions of two phenylalanine
ammonialyase isoforms (PAL1 and PAL2) and of cinnamate-4-hydroxylase
(Achnine et al., 2004). Moreover, the existence of a multi enzyme complex has
been proposed for the anthocyanin pathway in rice by yeast-two hybrid
experiments (Shih et al., 2008).
Most of the flavonoid synthesizing enzymes are recovered in soluble cell
fractions, immune localization experiments suggest that they are loosely bound to
the endoplasmic reticulum (ER), possibly in a multi-enzyme complex, whereas
the pigments themselves accumulate in the vacuole (i.e., anthocyanins and proanthocyanidins) or the cell wall (i.e., phlobaphenes, (Winkel-Shirley, 2001).
Flavonol synthase1 has recently been localized in Arabidopsis nuclei (Kuhn et
al., 2011), as well as chalcone synthase and chalcone isomerase (Saslowsky et
al., 2005). Interestingly, Antirrhinum majus aureusidin synthase, the enzyme that
catalyzes aurone biosynthesis from chalcones, was localized in the vacuole, while
the chalcone 4'-O-glucosyltransferase is localized in the cytoplasm, indicating
that chalcones 4-O-glucosides are transported to the vacuole and the rein
converted to aurone 6-O-glucosides (Ono et al., 2006). Moreover, a flavonoid- 3hydroxylase has been recently localized in the tonoplast in the hilum region of
the soybean immature seed coat (Toda et al., 2012).
Two models have been proposed for the mechanism of anthocyanin transport
from the ER to the vacuole storage sites: the ligandin transport and the vesicular
transport (Grotewold and Davis, 2008; Zhao and Dixon, 2010). The ligandin
transport model is based on genetic evidence showing that glutathione transferase
(GST)-like proteins are required for vacuolar sequestration of pigments in maize,
petunia and Arabidopsis (AtTT19) (Marrs et al., 1995; Alfenito et al., 1998).
The vacuolar sequestration of anthocyanins in maize requires a multidrug
resistance associated protein-type (MRP) transporter on the tonoplast membrane,
which expression is co-regulated with the structural anthocyanin genes
(Goodman et al., 2004). MRP proteins are often referred as glutathione S-X
(GS-X) pumps because they transport a variety of glutathione conjugates.
However, because anthocyanin–glutathione conjugate(s) have not been found, it
is proposed that these GSTs might deliver their flavonoid substrates directly to
the transporter, acting as a carrier protein or ligandin (Koes et al., 2005).
This hypothesis is supported by the fact that Arabidopsis’ GST (TT19), localized
both in the cytoplasm and the tonoplast, can bind to glycosylated anthocyanins
and aglycones but does not conjugate these compounds with glutathione (Sun et
al., 2012). The vesicle-mediated transport model proposed is based on
observations that anthocyanins and other flavonoids accumulate in the cytoplasm
in discrete vesicle-like structures (anthocyanoplasts), and then they might be
imported into the vacuole by an autophagic mechanism (Pourcel et al., 2010).
Nevertheless, grape vesicle-mediated transport of anthocyanins involves a GST
and two multidrug and toxic compound extrusion-typetransporters
(anthoMATEs). Thus, these observations point out to the coexistence of both
mechanisms of transports, in which the participation of GSTs and transporters
would be specific to cell and/or flavonoid-type (Gomez et al., 2011).
Biosynthesis genes of flavonoid regulated by the interaction of different families
of transcription factors (Falcone Ferreyra et al., 2012). Genes involved in the
anthocyanin pathway are differentially regulated in monocot and dicot species by
R2R3 MYB transcription factors, basic helix-loop-helix (bHLH), and WD40
proteins (Grotewold, 2005; Petroni and Tonelli, 2011). Thus, combinations of
the R2R3- MYB, bHLH, and WD40 transcription factors and their interactions
(MYB-bHLH-WD40 complex) determine the activation, and spatial and temporal
expression of structural genes of anthocyanin biosynthesis. The regulation of
anthocyanin biosynthesis in reproductive and other organs by MYB-bHLHWD40 complex has been reviewed (Petroni and Tonelli, 2011). There are
interesting differences in anthocyanin regulation between monocot and dicot
species like Arabidopsis and maize. In Arabidopsis, TT2, TT8, and TTG1 form a
ternary complex and activate pro-anthocyanidin biosynthesis in developing seeds,
while, TTG1, aWD40 transcription factor, different bHLH (TT8, GL3, and
EGL3) and MYB transcription factors (PAP1 and PAP2) interact to activate
anthocyanin synthesis in vegetative tissues (Figure 2A) (Baudry et al., 2004;
Feller et al., 2011).
In maize, MYB and bHLH proteins are encoded by two multi gene families
(PL/C1 and B/R, respectively), and each member has a tissue and developmental
specific pattern, while a WD40 protein PAC1 is required by both B1or R1
proteins for full activation of anthocyanin biosynthetic genes in seeds and roots
(Figure 2B) (Carey et al., 2004). Functional Arabidopsis TTG1 is required for
anthocyanin accumulation during roots and trichomes development (Galway et
al., 1994), and maize PAC1 can complement Arabidopsis ttg1 mutants, however,
maize pac1 mutants only show a reduction in anthocyanin pigmentation in
specific tissues (Carey et al., 2004). Even more, the regulation of flavonol
biosynthesis exhibit important differences between both species.
In Arabidopsis, three R2R3-MYB proteins, MYB12, MYB11, and MYB111
(PFG1-3), which exhibit differential spatial expression patterns, regulate AtFLS1
expression in a tissue and developmental specific manner (Stracke et al., 2007),
while, ZmFLS1/2 are regulated by both P1 (R2R3-MYB) and the anthocyanin
C1/PL1 and R/B regulators (Figure2) (Falcone Ferreyra et al., 2012).
Nevertheless, flavonols are essential for pollen germination and conditional male
fertility in maize (Mo et al., 1992; Taylor and Hepler, 1997), but maize plants
lacking the P1 and R/B+C1/PL1 anthocyanin regulators are fertile (Coe and
Neuffer, 1988; Dooner et al., 1991; Neuffer et al., 1997). In addition, a PFG13-independent flavonol accumulation occurs in pollen and siliques/seeds in
Arabidopsis (Stracke et al., 2010), suggesting that, in both species, additional
regulators, not yet identified, are also involved in the regulation of FLS
expression, and consequently, in flavonol accumulation. Inaddition, the evolution
of MYB and bHLH plant families has been deeply analyzed from structural and
functional perspectives (Feller et al., 2011). Interestingly, the identification of a
C1-like (MBF1) regulator in the gymnosperm Picea mariana (black spruce)
further supports the idea that the regulation of anthocyanin pathway by a C1-like
class of R2R3 MYB protein precedes the evolutionary separation of angiosperms
from gym- no sperms (Xue et al., 2003).
The identification of both bHLH and MYB proteins in mosses further supports
the hypothesis that the bHLH–MYB complex has evolved early during land plant
evolution (Pires and Dolan, 2010). Many R2R3 MYB transcription factors were
first identified from several model plants, such as maize, Antirrhinum, petunia,
and Arabidopsis. These transcription factors are involved in the regulation of the
flavonoid biosynthesis pathway.
Inspite of the fact that generly flavonoids are produced in plants as a secondery
metabolites with varying concenterations, yet medicinal and aromatic plants are
known to be more efficient in producing these substances that can be extracted in
a commercial quantities using developed techniques.
459
J Microbiol Biotech Food Sci / Alia Amer 2018 : 7 (5) 457-468
Flavonoids occurring virtually in all plant parts, particularly the
photosynthesizing plant cells. They are a major colouring component of
flowering plants. Flavonoids are an integral part of human and animal diet. Some
food sources containing different classes of flavonoids are given in Table 2.
Being phytochemicals, flavonoids cannot be synthesized by humans and animals
(Koes et al., 2005). Thus flavonoids found in animals are of plant origin rather
than being biosynthesized in situ. Flavonols are the most abundant flavonoids in
foods. Flavonoids in food are generally responsible for colour, taste, prevention
of fat oxidation, and protection of vitamins and enzymes (Yao et al., 2004).
Flavonoids found in the highest amounts in the human diet include the soy
isoflavones, flavonols, and the flavones. Although most fruits and some legumes
contain catechins, the levels vary from 4.5 to 610mg/kg (Arts et al., 2000).
Preparation and processing of food may decrease flavonoid levels depending on
the methods used. For example, in a recent study, orange juices were found to
contain 81–200mg/L soluble flavanones, while the content in the cloud was 206–
644 mg/L which suggest that the flavanones are concentrated in the cloud during
processing and storage (Gil-Izquierdo et al., 2001). Accurate estimation of the
average dietary intake of flavonoids is difficult, because of the wide varieties of
available flavonoids and the extensive distribution in various plants and also the
diverse consumption in humans (Tom´as-Barber´an and Clifford, 2000).
Table 2 Some dietary flavonoids sources and its classification as well as
structure
Class
Flavonoid
Dietary source
References
(+)-Catechin
Flavanol
(Lopez et
(−)-Epicatechin
Tea
al.,2001)
Epigallocatechin
Chrysin, apigenin
Fruit skins, red
(Hara et al.,1995;
Rutin, luteolin,
wine,
Flavone
Kreftet al., 1999;
and
buckwheat, red
Stewart et al.,
luteolin
pepper, and
2000; Hertog et
glucosides
tomato skin
al., 1992).
Kaempferol,
Onion, red
Flavonol
(Stewart et al.,
quercetin,
wine, olive oil,
2000)
myricetin, and
berries, and
tamarixetin
grapefruit.
Naringin,
Citrus fruits,
(Miyake et
Flavanone
naringenin,
grapefruits,
al.,2000;
taxifolin,
lemons, and
Rousseff et al.,
1987)
and hesperidin
oranges
(Reinli and
Isoflavone
Genistin, daidzin
Soyabean
Block, 1996)
Cherry,
(Stewart et al.,
Apigenidin,
Anthocyanidin
easberry, and
2000; Hertog et
cyanidin
al., 1992).
strawberry
Figure 2 Regulation of the flavonoid pathway in Arabidopsis thaliana (A) and
maize (B). Enzymes and intermediates are indicated in black and different
regulators are indicated in colour. The end products are identified in capital
letters. Dotted arrows indicate multiple steps. CHS, Chalcone synthase, CHI,
chalcone isomerase, F3H, flavanone3-hydroxylase, F3_H, flavonoid-3_ hydroxylase, DFR, dihydro flavonol4- reductase, FNR, flavanone4-reductase,
ANS, anthocyanidin synthase, UFGT, UDP-glucose flavonoid3-Oglucosyl
transferase, FLS, flavonol synthase, LAR, leuco anthocyanidin reductase, ANR,
anthocyanidin reductase. (See: Falcone Ferreyra et al., 2012)
MEDICINAL PLANTS AS A SOURCE OF FLAVONOIDS
Plants plays an important part in our everyday diet, In addition to essential
primary metabolites (e.g. carbohydrates, lipids and amino acids), higher plants
are also able to synthesize a wide variety of low molecular weight compounds.
Plant secondary metabolites can be defined as compounds that have no
recognized role in the maintenance of fundamental life processes in the plants
that synthesize them, but they do have an important role in the interaction of the
plant with its environment. The production of these compounds is often low (less
than 1% dry weight) and depends greatly on the physiological and developmental
stage of the plant (Dixon, 2001; Oksman-Caldentey and Inzé, 2004).
Verpoorte et al., (1999) reported that the plants synthesize a remarkably diverse
collection of chemicals. Quite notably, tremendous diversity is observed among
“secondary” metabolites, a large group of compounds that until recently had been
regarded to be not completely paramount to plant survival. These are the
compounds that have emerged through evolution as the bulk of the dynamic
chemical vocabulary underlying plant-environment interaction. A recent estimate
has put the total number of plant secondary metabolites at 100,000 compounds,
with an additional 4,000 being discovered annually.
Flavonoids are widely distributed throughout the plant kingdome and about 3000
varieties of flavonoids are known (Kunhan, 1976). Many have low toxicity in
mammals and some of them are widely used in medicine (Cesarone et al., 1992).
Recently there has been an up surge of interest in the therapeutic potential of
medicinal plants which might be due to their phenolic compounds, specifically to
flavonoids (Pourmorad et al., 2006; Kumar and Pandey, 2012). Flavonoids
have been consumed by humans since the advent of human life on earth, that is,
for about 4 million years. They have extensive biological properties that promote
human health and help reduce the risk of diseases. Oxidative modification of
LDL cholesterol is thought to play a key role during atherosclerosis. The
isoflavan glabridin, a major polyphenolic compound found in Glycyrrhiza glabra
(Fabaceae), inhibits LDL oxidation via a mechanism involving scavenging of
free radicals (Fuhrman et al., 1997). Several epidemiologic studies have
suggested that drinking either green or black tea may lower blood cholesterol
concentrations and blood pressure, thereby providing some protection against
cardiovascular disease. Flavonoids are also known to influence the quality and
stability of foods by acting as flavorants, colorants, and antioxidants (Craig,
1999; Kumar et al., 2012). Flavonoids contained in berries may have a positive
effect against Parkinson’s disease and may help to improve memory in elderly
people. Antihypertensive effect has been observed in total flavonoid fraction of
Astragalus complanatus in hypertensive rats (Li et al., 2005). Intake of
antioxidant flavonoids has been inversely related to the risk of incidence of
dementia (Commenges et al., 2000).
Table 3 summarizes some of the medicinal plants rich in flavonoid contents.
Solubility may play major role in the therapeutic efficacy of flavonoids. Low
solubility of flavonoid aglycones in the water coupled with its short residence
time in the intestine as well as its lower absorption does not allow humans to
suffer acute toxic effects from the consumption of flavonoids, with the exception
of a rare occurrence of allergy. The low solubility of the flavonoids in water often
presents a problem for its medicinal applications. Hence, the development of
semisynthetic, water-soluble flavonoids, for example, hydroxyethylrutosides and
inositol-2-phosphatequercetin, has been implicated in the treatment of
hypertension and micro bleeding (Havsteen, 2002).
460
J Microbiol Biotech Food Sci / Alia Amer 2018 : 7 (5) 457-468
Table 3 Some Medicinal plants as a source of flavonoids
Plant
Plant
Family
(scientific name)
(Common name)
Aloe vera
Aloe
Asphodelaceae
Acalypha indica
Indian acalypha
Euphorbiaceae
Azadirachta indica
Neem
Meliaceae
Bacopa moneirra
water hyssop
Scrophulariaceae
Betula pendula
silver birch
Betulaceae
Butea monospermea
flame-of-the-forest
Fabaceae
Bauhinia monandra
orchid tree
Fabaceae
Brysonima crassa
locustberries
Malphigaceae
Calendula officinalis
marigold
Compositae
Cannabis sativa
cannabi
Compositae
Citrus medica
Lemon
Rutaceae
Clitoria ternatea
butterfly pea
Fabaceae
Glyccheriza glabra
Liquorice
Leguminosae
Mimosa pudica
Sleepy (shy) plant
Mimosoideae
Mentha longifolia
mint
Lamiaceae
Momordica charantia
bitter melon
Curcurbitaceae
Oroxylum indicum
midnight horror,
Bignoniaceaea
Passiflora incarnate
Purple passionflower Passifloraceae
Pongamia pinnata
Pongame oiltree
Fabaceae
Tephrosia purpurea
Fish poison
Fabaceae
Tilia cordata
leaf linden-little
Tiliaceae
BIOTECHNOLOGY APPROACHES FOR FLAVONOIDS PRODUCTION
FROM PLANTS
Callus and cell suspension culture
Plant cell culture systems represent a potential renewable source of valuable
medicinal compounds, flavors, fragrances, and colorants, which cannot be
produced by chemical synthesis (Vanisree and Hsin-Sheng, 2004). The
capability to cultivate plant callus cells and organs in liquid media has also made
an important contribution to modern plant biotechnology with respect to the
production of commercially valuable compounds. (Su and Lee, 2007). The
homogeneity of an in vitro cell population, the large availability of material, the
high rate of cell growth and the good reproducibility of conditions make
suspension cultured cells suitable for the analysis of complex physiological
processes at the cellular and molecular levels. Moreover, plant cell cultures
provide a valuable platform for the production of high-value secondary
metabolites and other substances of commercial interest. (Moscatiello et al.,
2013). Callus and cell suspension cultures have been carried out in several plants
for the production of flavonoids. Agarwal and Kamal (Agarwal and Kamal,
2007) studied the total flavonoid content in Momordica charantia and observed
that the maximum amount of total flavonoid (1.83 mg/l dry wt.) accumulated in
6-wk-old callus. The embryogenic callus and suspension culture of Iphiona
mucronata showed the presence of flavonoid content but the regenerated plantlets
were devoid of it. (Al-Gendy et al., 2013) Callus culture was also studied for the
isolation and detection of quercetin in Pluchea lanceolata. (Arya et al., 2008)
Alfalfa callus culture was established and total flavonoids concentration was
studied by (Khalil et al., 2008; Alia, 2008), the results showed that the leaf callus
produced the highest level of flavonoid with approximately (170 µg/mg fresh
weight). Cheel et al. (2007) working in vitro culture of Sanicula graveolens
found that on dry weight basis, total flavonoid content ranged from 1.23% to
2.23% being lower for the root culture.. Chen et al. (2006) reported that the
callus growth quantity in Cyclocarya paliurus [Pterocarya sp.] was higher in stem
than that in the leaf, but the flavonoid content in the leaf was higher than that in
the stem and the optimual plant growth regulator combination promoting the
callus growth and flavonoid content accumulation was 1.0 mg l-1 kinetin + 0.5 mg
l-1 2, 4- D + 0.3 mg l-1 NAA. These results are in agreement with (Yamamoto et
al., 1986) who mentioned that the growth and flavonoid (baicalin, baicalein,
wogonin and wogonin-7-0-glucuronide) content of the St-20 line of Scutellaria
baicalensis callus were best on a medium containing 10-7 to 10-5M kinetin. After
culture for 70 days the St-20 line had a similar flavonoid content and pattern to
that of the parent plant roots. Also, (Chen and Cao, 2007) observed that
flavonoid content in the callus of Ginkgo biloba from different explants was
higher in root > leaf > cotyledon > stem. On the other hand, (Saker and
Kawashity, 1998), working on Nepeta and Plantago species endemic in Egypt,
found that the flavonoid contents of organized tissues, although about 3-times
greater than those of unorganized tissues (callus), were still lower than those of
the original plants (control). Similar results were found on Lotus tenuis Waldst by
(Strittmatter et al., 1991) who reported that flavonoids were not detected in vitro
callus cultures, but flavonoid production in plantlets derived from the callus
showed similar patterns to the field-grown plants. Pasqua et al. (1991)
suggested that flavonoid production in Maclura pomifera was markedly higher
from cell cultures, although the composition was similar for calluses and cell
cultures. Tadhani et al, (2007) showed that the flavonoids content in Stevia
rebaudiana was found to be 21.73 and 31.99 mg / g in the leaf and callus,
Flavonoid
References
Luteolin
Kaempferol glycosides
Quercetin
Luteolin
Quercetrin
Genistein
Quercetin-3-O-rutinoside
(+)-catechin
isorhamnetin
Quercetin
hesperidin
kaempferol-3-neohesperidoside
Liquiritin,
Isoquercetin
Luteolin-7-O-glycoside
Luteolin
Chrysin
Vitexin
Pongaflavonol
Purpurin
hyperoside
(L´azaro, 2009)
(L´azaro, 2009)
(Tripoli et al., 2007)
(L´azaro, 2009)
(Gupta et al., 1983)
(Murlidhar et al., 2010)
(Murlidhar et al., 2010)
(Aderogba et al., 2006)
(Gupta et al., 1983)
(Guptaet al.,1983)
(L´azaro, 2009)
(Sankaranarayanan et al., 2010)
(Gupta et al., 1983)
(Sannomiya et al., 2005)
(Kogawaet al., 2007)
(Ghoulami et al., 2001)
(Sannomiya et al., 2005)
(Gupta et al.,1983)
(Agarwal and Kamal, 2007)
(Sannomiya et al., 2005)
(Guptaet al.,1983)
respectively. Li et al., (2004) working on Eucommia ulmoides plant found that
flavonoid contents were highest in hypocotyl calluses.
Madhavi et al. (1998) studied the isolation of bioactive constituents from
Vaccinium myrtillus fruits and cell cultures. Major fractions contained
flavonoids, such as cyanidin-3- galactoside, cyanidin-3-glucoside, cyanidin-3arabinoside and proanthocyanidins. Anthocyanin accumulation in callus was
lower than in the fruit. Callus cultures accumulated proanthocyanidins were
similarly present in fruit extracts (oligo- and polymeric. Dias et al. (1998)
published the isolation of a new naturally occurring compound 6-C-prenyl
luteolin, together with luteolin-5,3’-dimethyl ether, luteolin-5-glucoside and
luteolin-3’-glucoside from the callus of Hypericum perforatum var.
angustifolium. The total flavonoid content of callus was much lower than that
found in wild growing H. perforatum plants.
Fedoreyev et al. (2000) established callus cultures from the different parts of
Maackia amurensis and analysed for isoflavonoids. The isoflavones daidzein,
retuzin, genistein and for mononetin and the pterocarpans maakiain and
medicarpin were found to be produced by these cultures. The content of
isoflavones and pterocarpans was essentially the same in cultures derived from
leaf petioles, inflorescences and apical meristems of the plant. The maximal yield
of isoflavones and pterocarpans in calluses approximately four times higher than
the content of the heartwood of M. amurensis plants. Moreover, (Łuczkiewicz
and Głod, 2003; Luczkiewicz et al., 2014) established six callus cultures and
studied the effect of plant growth regulators of Genista species with the objective
to produce isoflavones of phytoestrogenic activity. The cultures were optimized
for their growth and isoflavonoid production by changing various media in the
presence or absence of light. The best growth and the highest isoflavone
production was obtained under constant light regime on SH basal medium
containing 22.6 µmol/L 2,4-dichlorophenoxyacetic acid (2,4-D), 23.2 µmol/L
kinetin. Callus cultures of all species produced more isoflavones than the parent
herbs.
Stable and optimized callus cultures are a logical step in the first phase of the cell
culture production of plant secondary metabolites, i.e. preparing the inoculum for
liquid suspension cultures. Production of flavonoids in cell suspension cultures
have been widely published and it was proposed as a technology to overcome
problems of variable product quantity and quality from whole plants due to the
effects of different environmental factors, such as climate, diseases and pests
(Yamamoto et al., 1995, Zhang et al., 1997; Zhang et al., 2002; Rao and
Ravishankar, 2002; Yamamoto et al., 2004).
During the past decades, this technology attracted much academic and industrial
interest. The approach of using plant cell suspension cultures for secondary
metabolite (including flavonoids) production is based on the concept of
biosynthetic totipotency of plant cells (Rao and Ravishankar, 2002), which
means that each cell in the cultures retains the complete genetic information for
production of the range of compounds found in the whole plant. Cell suspension
cultures are initiated from established callus cultures by inoculating them into
liquid media. The cultures are then kept in glass flasks under continual agitation
on horizontal or gyratory shakers and eventually they can be transferred to a
specialized bioreactor (Bourgaud et al., 2001). There have been examples of
successful production of some compounds from this group of metabolites, for
instance, (Yamamoto et al., 1995) showed the effect of polysaccharides on the
production of prenylated flavanones (sophoraflavanone G and lehmanin) in
Sophora flavescens callus culture. The production of these flavanones was
stimulated up to 5 times by addition of 2 mg/mL yest extract. Moreover, the
461
J Microbiol Biotech Food Sci / Alia Amer 2018 : 7 (5) 457-468
production of prenylated flavanones also can be increased by 2-5 times by
addition of cork pieces (Yamamoto et al., 1996).
Another authors (Delle Monache et al., 1995) isolated flavonoids from callus
and cell cultures of Maclura pomifera. Among the flavonoids, flavones and
flavanones were produced preferentially by suspended cells, but with the prenyl
substituents exclusively on ring A, while the isoflavones did not show the 3’, 4’dihydroxyl substitution pattern found in the products isolated from fruits. The M.
pomifera cell suspension culture showed a greater level of metabolite
accumulation (0.91%) than stems (0.26%), leaves (0.32%) and fruits (0.08%) of
the parent plant. (Zhang et al., 1997) studied the temperature effect on
anthocyanin production in cell suspension cultures of Fragaria ananassa at a
temperature range of 15-35◦ C. The maximum anthocyanin production was
obtained at 20◦ C. Anthocyanin production of 270 mg/L on day 9 was increased
1.8, 3 and 4-fold over that of cultures at 20, 25 and 30 ◦ C, respectively.
In addition, recent phytochemical studies have documented the presence of some
phenolic acids and flavonoids in fruit extracts (Mocanetal.,2016; Mocanet al.,
2016; Mocanet al.,2014). Analyses of S. chinensis fruit extracts confirmed the
presence of chlorogenic, p-coumaric, p-hydroxybenzoic, protocatechuic, salicylic
and syringic acids (Szopa and Ekiert, 2012). Other authors have additionally
proved the presence of gentisic acid and flavonoids: hyperoside, isoquercitrin,
rutin and quercetin (Mocan et al., 2014).
Also, there have been different interest reports showed the successful production
of flavonoids as active ingredients, for instance, Rosmarinic acid in cultures in
vitro of many Lamiaceae and Boraginaceae species (Ekiert et al., 2013),
rosmarinic and chlorogenic acids in cell and organ cultures of Eryngium
planum (Kikowska et al., 2012), ellagic acid in shoot cultures of Rubus
chamaemorus (Thiem et al., 2003), protocatechuic acid in shoot cultures of Ruta
graveolens (Ekiert et al., 2009), and p-coumaric acid in shoot-differentiating
callus cultures of Ruta graveolens ssp. divaricata (Ekiert et al., 2014).
Furthermore, considerable amounts of flavonoids have been obtained in
cultures in vitro of plant species such as Astragalus missouriensis (Ionkova,
2009), Cyclopia genistoides (Kokotkiewicz et al., 2014), Hyoscyamus
muticus (Biondi
et
al.,
2002),
or Dionaea
muscipula and Drosera
capensis (Krolicka et al., 2008). Schisandra chinensis (Szopa et al., 2016a,b;
Szopa et al., 2017).
Hairy root culture
Transgenic hairy root cultures have revolutionized the role of plant tissue culture
in secondary metabolite production. They are unique in their genetic and
biosynthetic stability, faster in growth, and more easily maintained. Using this
methodology, a wide range of chemical compounds has been synthesized.
(Shanks and Morgan, 1999; Giri and Narasu, 2000) Hairy root cultures of
many plant species have been widely studied for the production of secondary
metabolites useful as pharmaceuticals, cosmetics, and food additives. (Christey
and Braun, 2005; Georgiev et al., 2007; Srivastava and Srivastava, 2007)
Hairy root cultures represent an interesting alternative to dedifferentiated cell
cultures for the production of secondary plant products. Because hairy roots
originate from a single plant cell infection by Agrobacterium rhizogenes, they are
usually considered as genetically stable, in contrast with callus lines.
Also, in contrast to dedifferentiated cells, the production of secondary
metabolites is not repressed during the growth phase of the culture. Therefore,
hairy roots usually produce secondary plant compounds without the loss of
concentration frequently observed with callus or cell suspension cultures.
(Bourgaud et al., 1997) Therefore hairy root cultures of seven Psoralea species
were established (Bourgaud et al., 1999) and the flavonoid (daidzein,
coumestrol), production was enhanced by using chitosan as elicitor. The effect of
rare earth element Praseodymium (Pr) on flavonoids production and its
biosynthesis was studied in Scutellaria viscidula hairy roots (Lei et al., 2011).
Zhang et al. (2009) reported that over a culture period of 3 weeks, the wild-type
hairy roots of G. uralensis, the untreated transgenic hairy roots, and the doubletreated transgenic hairy roots accumulated 0.842, 1.394, and 2.838 (g/100 g DW)
of total flavonoids, respectively. Moreover, the enhanced accumulation of
flavonoids was correlated with the elevated level of chi transcripts and CHI
activity, confirming the key role of chi in the flavonoids synthesis and they
demonstrated that the combination of the metabolic engineering and PEG8000YE elicitation treatment was an effective strategy to increase the flavonoids
production in hairy roots of G. uralensis Fisch.
Studies showed that compared to callus cultures, hairy roots from the 7 Psoralea
plant species (Leguminosae), displayed comparable concentrations of flavonoids.
However, high-producing lines were more frequently found with hairy roots (4
out of 18) than with callus cultures (4 out of 217) (Bourgaud et al., 1999).
Moreover, (Zhao et al., 2014) indicated that the F. tataricum hairy root culture
could be an effective system for rutin and quercetin production and the maximal
flavonoids yield was enhanced to 47.13 mg/L, about 3.2 fold in comparison with
the control culture of 14.88 mg/L.
Hairy root cultures of many plant species have already been widely studied
regarding the production of secondary metabolites which could be used as
pharmaceuticals, cosmetics, and food additives (Crane et al., 2006; Georgiev et
al., 2007, Thiruvengadam et al., 2014). Biotechnological approaches which
used hairy root culture have greatly enhanced the production of rutin by common
buckwheat (Lee et al., 2007; Kim et al., 2010) and the production of phenolic
compounds by tartary buckwheat (Kim et al., 2009; Thwe et al., 2013). Also
rutin and quercetin biosynthesis in Fagopyrum tataricum Gaertn (Huang et al.,
2016).
Elicitors and elicitation for flavonoids production
Until now, various strategies have been developed to improve the production of
secondary metabolites in vitro cultures, such as manipulating the parameters of
the environment and medium, selecting high yielding cell clones, precursor
feeding and elicitation (reviewed in Collin, 2001; Rao and Ravishankar, 2002;
Verpoorte et al., 2002).
This broader definition of elicitors includes both substances of pathogen origin
(exogenous elicitors) and compounds released from plants by the action of the
pathogen (endogenous elicitros). Elicitors are molecules of biological and
nonbiological origin that stimulate secondary metabolism synthesis and could
play an important role in biosynthetic pathways to enhanced production of
commercially important compounds (Dornenburg and Knorr, 1995).
Elicitiation can be used as one of the important strategies in order to get better
productivity of the bioactive secondary products (Chong et al., 2005;
Smetanska, 2008; Sharma et al., 2011; Hussain et al., 2012) and lowering
production costs. (Miao et al., 2000; Jian-Yong, 2003) Elicitors are compounds
stimulating any type of plant defense. (Radman et al., 2003) The secondary
metabolites are released due to defense responses which are triggered and
activated by elicitors, the signal compound of plant defence responses. (Patel
and Krishnamurthy, 2013) Copper sulphate as abiotic elicitor was used on the
production of flavonoids in cell cultures of Digitalis lanata. (Bota and Deliu,
2011) Callus cultures of Ononis arvensis with AgNO3 as an elicitor was used to
enhance flavonoid production. (Tumova and Polivkova, 2006). In addition a
wide variety of elicitors, such as fungal elicitors, methyl jasmonate, benzoic acid
and arachidonic acid can induce the biosynthesis of secondary metabolites
(Yukimune et al., 1996).
Legumes such as bean, soybean, chickpea, and alfalfa (Medicago sativa)
response to elicitation in the accumulation of antimicrobial isoflavonoid
phytoalexins (Kessmann et al., 1990). In alfalfa cell-suspension cultures elicitorinduced accumulation of the isoflavonoid phytoalexin medicarpin is preceded by
increases in the extractable activities of all enzymes involved in its biosynthesis
L-Phenylalanine (Kessmann et al., 1990). Previous work on the relationship
between gene transcription and subsequent metabolic events in elicitor treated
alfalfa cells has demonstrated a correlation between an increased transcription
rate and subsequent increases in enzymatic activity for a range of genes involved
in the core phenylpropanoid pathway and the flavonoid isoflavonoid branch
pathway (Kessmann et al., 1990). Also Yeast extract (YE) elicitor treatment
during the exponential growth phase showed a significant flavonoid induction
than during the stationary growth phase. aslo Jasmonic acid affecting the
production of flavonoids in alfalfa suspension culture (Khalil et al., 2008; Alia,
2008). Dixon et al. (1995) showed that the isoflavonoid conjugates medicarpin-30-glucoside-6"- O-malonate (MGM), afrormosin-7-O-glucoside (AG), and
afrormosin-7-O-glucoside-6"-O-malonate
(AGM)
were
isolated
and
characterized from cell suspension cultures of alfalfa (Medicago sativa L.), where
they were the major constitutive secondary metabolites. They were also found in
alfalfa roots, but not in other parts of the plant. The phytoalexin medicarpin
accumulated rapidly in suspension cultured cells treated with elicitor from
Colletotrichum lindemuthianum, and this was subsequently accompanied by an
increase in the levels of MGM.
Mizukami et al. (1993) and Szabo et al. (1999) reported that the jasmonates
have been shown to induce rosmarinic acid and shikonin production in cell
cultures of Coleus blumei and Lithospermum erythrorhizon, respectively. They
have also been reported to play an important role in signal transduction processes
that regulate defence genes in plants during assaults such as insect feeding
(Farmer and Ryan, 1990; Walling, 2000). In addition, JA and methyl
jasmonate increase the production of hypericin in cell suspension cultures of H.
perforatum (Travis et al., 2002; Jing et al., 2015). Moreover Yamamoto et al.
(2004) showed that some elicitors such as methyl jasmonate and yeast extract
stimulated the production of sophora flavanone G (SFG) in cultured cells of
Sophora flavescens.
Flavonoids are produced as protective substances against UV-B radiation in
plant. As an effective abiotic elicitor, some studies have described the production
of flavonoids by buckwheat sprouts in response to UV-B irradiation (Kreft et al.,
2002; Eguchi and Sato, 2009). Rutin (sometimes called vitamin P) displays
strong antioxidant activity which could alleviate the damage from UV-B
stress. Tsurunaga et al. (2013) found that rutin content and radical scavenging
activity of buckwheat sprouts were enhanced under various levels of UV-B
radiation.
Huang et al. (2016) reported that rutin and quercetin content of hairy roots and
all parts of tartary buckwheat were increased under UV-B stress. The maximal
increase of rutin content (from 3.19 to 29.79 mg g-1, 9.35-fold) was observed in
leaves. Interestingly, the next-highest increase of rutin content (from 0.93 to 4.82
462
J Microbiol Biotech Food Sci / Alia Amer 2018 : 7 (5) 457-468
mg g-1, 5.18-fold) was observed in hairy roots. In a previous study of
buckwheat, (Kim et al., 2010) found that rutin content was ∼2.4-fold higher in
hairy roots than in WT roots. These findings are consistent with those of
transformation
studies
on
other
plants,
which
suggested
that Agrobacterium transfection might greatly enhance rutin content (Fu et al.,
2006). According previous work, some work indicated that biotic elicitors can
also enhance rutin and quercetin production in F. tataricum hairy root, e.g., Yeast
polysaccharide (Zhao et al., 2014) and exogenous fungal mycelia (Zhao et al.,
2014b).
The elicitors can be biological or chemical in origin. The yeast elicitor,
Saccharomyces cereviseae increased the production of berberine by 4-folds in
Thalictrum rugosum. Rajendran et al. (1994) observed 3-fold elicitation of
anthocyanin by Aspergillus flavus mycelial extract in cultured cells of Daucus
carota. Kang et al. (2006) studied the effect of the elicitor salicylic acid (SA) on
the production of bilobalide, ginkgolide A (GA), and ginkgolide B (GB) in cell
suspension cultures of Ginkgo biloba. Buitelaar et al. (1992) reported 85%
increase in thiophene production with Aspergillus niger elicitor whereas it was
55% with Penicillium expansum elicitor in the hairy roots of Tagetes patula. Cell
suspension cultures of Taxus chinensis, treated with 20, 40 and 100 mg /L
Aspergillus niger elicitor showed 5, 8 and 3-fold increase in taxol production
than that of the control (Lan et al., 2003). Mendhulkar et al. (2016) indicated
that for flavonoid elicitation in Blumea lacera, Aspergillus niger is more
responsive than Salicylic acid. Also Yeast extract (YE) elicitor treatment during
the exponential growth phase showed a significant flavonoid induction than
during stationary growth phase. YE at 1 g l-1 with culture harvested on day 12
were the best treatment affecting the production of flavonoid (Alia, 2008).
Nano treatments for flavonoids enhancement
The phenomenal surface characteristics of Nanoparticles (NP) attribute to its
extraordinary and unique properties. By increasing the number of atoms on
surface, there is an increase in total free energy, resulted in the alteration of
material characteristics. Nanoparticles have the potential to be used as novel
effective elicitors in plant biotechnology for the elicitation of secondary
metabolite production (Fakruddin et al., 2012). Many researchers have studied
the role of NPs as elicitors (Aditya et al., 2010; Asghari et al., 2012; Sharafi et
al., 2013; Zhang et al., 2013; Ghanati and Bakhtiarian, 2014; Raei et al.,
2014; Ghasemi et al., 2015; Yarizade and Hosseini, 2015). A number of
studies have supported the possible role of NPs as elicitors for enhancing the
expression level of genes related to the production of secondary metabolite
(Ghasemi et al., 2015; Yarizade and Hosseini, 2015). Nanoparticles have
successfully offered a new strategy in enhancing the secondary metabolite
production. But still an in-depth and consolidate insight in research is required to
elucidate the effects of NPs in production mechanisms of secondary metabolite
production in medicinal plants (Misra et al., 2016).
Flavonoids and isoflavonoids are the most popular groups of secondary
metabolites found in plants. Many legume seeds have been reported to be rich
sources of these secondary metabolites (Heiras-Palazuelos et al., 2013). ALOubaidi and Kasid (2015) demonstrated the increased production of secondary
metabolite (phenolic and flavonoid compounds) in gram on exposure to TiO2 NPs
under in vitro condition. Secondary metabolite contents in the callus were
estimated qualitatively and quantitatively using HPLC and compared with the
mother plant. TiO2 NPs at varying concentrations (0.5, 1.5, 3, 4.5, 6) mg L−1
were used for an effective increase in secondary metabolites. The results revealed
that the secondary metabolite concentration from callus embryo of gram
increased to a highly significant level at the concentrations of 4.5 and 6.0 mg L-1.
The HPLC outcomes confirmed the elevation in the secondary metabolite level
under the effect of the TiO2 NPs when compared with the mother plant. In a very
recent report, Khan et al., (2016) examined the effect of nine types of metal
nanoparticles including monometallic and bimetallic alloy nanoparticles [Ag, Au,
Cu, AgCu (1:3), AgCu (3:1), AuCu (1:3), AuCu (3:1), AgAu (1:3), AgAu (3:1)]
on total phenolic and flavonoid contents in milk thistle plant. The sterilized seeds
were soaked in NPs suspensions for 2 h and allowed to grow under in vitro
condition. The experiment was conducted for 6 weeks, and samples for total
phenolic and flavonoid contents were collected on a weekly interval. NPs
suspensions affected total phenolic and flavonoid contents in the plant in a
different way. It was observed that the amount of phenolics and flavonoids did
not show any correlation with the total dry mass of the plant.
However, duration of the experiment significantly affected the amount of total
flavonoids and phenolics in milk thistle. After 21 days presoaking of seeds in
bimetallic alloy, enhanced whereas monometallic NPs suspensions, reduced
phenolics and flavonoids content in milk thistle plantlets. After 28 days, Au and
Cu NPs caused maximum total phenolic and flavonoid accumulation in milk
thistle plants. Therefore, the maximum effect on secondary metabolites was
recorded with monomatellic NPs. Mainly three factors (size, surface area, and
composition of NPs) played a significant role either singly or in combination.
Plants are the main repository of all kinds of biochemicals which are produced as
primary and secondary metabolites. Secondary metabolites are industrially
important as they constitute the major chunk of pharmaceutically important
drugs. As a result of their huge demand in modern market they are overexploited
from their natural habitat, resulting in the disappearance of many plant species.
Therefore, Biotechnology offers different in vitro systems and have been
developed to exploit these active ingredients such as, in callus cultures, cell
suspension cultures hairy root cultures and nanoparticles which are the emerging
fields of biotechnology to investigate and enhance the production of these
products.
This review briefly summarized the flavonoids chemistry and biosynthesis as one
of the most important secondary compounds found in medicinal plants, as well as
the possible sources of flavonoids for their perspective biotechnological
production. Flavonoids are a large group of low-molecular weight polyphenolic
secondary metabolites, Fruits and vegetables are natural sources of flavonoids.
The basic flavonoid structure is aglycone. Flavonoids are synthesized through the
phenylpropanoid pathway, transforming phenylalanine into 4-coumaroyl- CoA,
which finally enters the flavonoid biosynthesis pathway which is regulated by the
interaction of different families of transcription factors.
Plant tissue cultures are being potentially used as an alternative new strategy for
industrial production of flavonoids, the production of flavonoids via tissue
culture techniques have been reported in both callus and cell suspension cultures.
The spectrum of the produced compounds and their yields depended on the
proper selection of plant species, explant types and culture conditions.
Biotechnological approaches which used hairy root culture have greatly enhanced
the production of many flavonoids compound which usually produce flavonoid
compounds without the loss of concentration frequently observed with callus or
cell suspension cultures. Therefore hairy root cultures represent an interesting
alternative to dedifferentiated cell cultures for the production of plant flavonoids.
Because hairy roots originate from a single plant cell infection by Agrobacterium
rhizogenes, they are usually considered as genetically stable, in contrast with
callus lines.
The most recent techniques is the use of nanoparticles for the elicitation of
secondary metabolite production as novel effective elicitors in plant
biotechnology. Nanoparticles have successfully offered a new strategy in
enhancing the secondary metabolite production. But still an in-depth and
consolidate insight multi desciblinary research research is required to elucidate
the effects of NPs in production mechanisms of secondary metabolite synthsis in
medicinal plants.
REFERENCES
Achnine L., Blancaflor E.B., Rasmussen S. & Dixon R.A. (2004). Colocalization
of L-phenylalanineammonia-lyase andcinnamate4-hydrozylasefor metabolic
channeling in phenyl- propanoid biosynthesis. Plant Cell, 16(11): 3098–3109.
http://dx.doi.org/10.1105/tpc.104.024406
Aderogba M.A., Ogundaini A.O. & Eloff J.N. (2006). Isolation of two flavonoids
from Bauhinia monandra leaves and their antioxidative effects. The African
Journal of Traditional, Complementary and Alternative Medicines, 3(4):59–65.
http://dx.doi.org/10.4314/ajtcam.v3i4.31177
Aditya N., Patnakar S., Madhusudan B., Murthy R. & Souto E. (2010).
Artemether loaded lipid nanoparticles produced by modified thin film hydration:
pharmacokinetics, toxicological and in vivo antimalarial activity. Eur J. Pharm.,
Sci., 40: 448–455. https://doi.org/10.1016/j.ejps.2010.05.007
Agarwal M. & Kamal R. (2007). Studies on flavonoid production using in-vitro
cultures of Momordica charantia. Indian Journal of Biotechnology, 6(2): 277–
279.
Agati G., Azzarello E., Pollastri S. & Tattini M. (2012). Flavonoids as
antioxidants in plants: location and functional significance. Plant Science, 196:
67–76. https://doi.org/10.1016/j.plantsci.2012.07.014
Alfenito M.R., Souer E., Goodman C.D., Buell R., Mol J., Koes R. & Walbot V.
(1998). Functional complementation of anthocyanin sequestration in the vacuole
by widely divergent glutathione S-transferases. Plant Cell, 10: 1135–1150.
https://doi.org/10.2307/3870717
Al-Gendy A.A., Bakr R.O. & El-gindi O.D. (2013). Somatic embryogenesis and
plant regeneration from callus and suspension cultures of Iphiona mucronata
(Forssk). European Sci. J., 9(27): 37-49.
Alia A.A. (2008). Physiological and biochemical studies on the production of
flavonoids from Medicago sativa through plant tissue culture. Masters’ thesis.
Faculty of Agriculture, Cairo Univ. Egypt.
AL-Oubaidi H.K.M. & Kasid N.M. (2015). Increasing (phenolyic and flavonoids
compounds of Cicer arietinum L. from embryo explant using titanium dioxide
nanoparticle in vitro. World J. Pharmaceut Res., 4(11):1791–1799.
Andrae-Marobela K., Ghislain F.W., Okatch H. & Majinda R.R. (2013).
Polyphenols: A diverse class of multi-target anti-HIV-1 agents. Current Drug
Metabolism, 14(4): 392–413. https://doi.org/10.2174/13892002113149990095
CONCLUSION
463
J Microbiol Biotech Food Sci / Alia Amer 2018 : 7 (5) 457-468
Arts I.C.W., Putte, V.B. & Hollman, P.C.H. (2000). Catechin contents of foods
commonly consumed in the Netherlands. Fruits, vegetables, staple foods and
processed foods, Journal of Agricultural and Food Chemistry, 48(5): 1746–
1751. https://doi.org/10.1021/jf000025h
Arya D., Patni, V. & Kant, U. (2008). In vitro propagation and quercetin
quantification in callus cultures of Rasna (Pluchea lanceolata Oliver & Hiern).
Indian J. Biotechnol., 7: 383-387.
Asghari G.H., Mostajeran A., Sadeghi H. & Nakhaei, A. (2012). Effect of
salicylic acid and silver nitrate on taxol production in Taxus baccata. J. Med.
Plants, 11(8):74–82.
Baudry A., Heim M.A., Dubreucq B., Caboche M., Weisshaar, B. & Lepiniec, L.
(2004). TT2, TT8, and TTG1 synergistically specify the expression of
BANYULS and pro-anthocyanidin biosynthesis in Arabidopsis thaliana. Plant J.,
39: 366–380. https://doi.org/10.1111/j.1365-313X.2004.02138.x
Biondi S., Scaramagli S., Oksman-Caldentey K.-M. & Poli F. (2002). Secondary
metabolism in root and callus cultures of Hyoscyamus muticus L.: the
relationship between morphological organisation and response to methyl
jasmonate. Plant Sci., 163: 563–569. https://doi.org/10.1016/s01689452(02)00161-9
Bota C. & Deliu C. (2011). The effect of copper sulphate on the production of
flavonoids in Digitalis lanata cell cultures. Farmacia, 59(1): 113-118.
Bourgaud F., Bouque V. & Guckert A. (1999). Production of flavonoids by
Psoralea hairy root cultures. Plant Cell, Tissue and Organ Culture, 56: 97–104.
https://doi.org/10.1023/a:1006206104795
Bourgaud F., Bouque V., Gontier, E. & Guckert A. (1997). Hairy root cultures
for the production of secondary metabolites. Ag. Biotech. News and Information,
9(9): 205–208.
Bourgaud F., Gravot A., Milesi S. & Gontier E. (2001). Production of plant
secondary metabolites: a historical perspective. Plant Sci., 161(5): 839–851.
https://doi.org/10.1016/s0168-9452(01)00490-3
Bowles D., Isayenkova J., Lim E. K. & Poppenberger B. (2005). Glycosyl
transferases: managers of small molecules. Curr. Opin. Plant Biol., 8: 254–263.
https://doi.org/10.1016/j.pbi.2005.03.007
Buslig B.S. & Manthey J.A. (2002). Flavonoids in cell function. Kluwer
Academic/Plenum Publishers Eds, New York, NY. pp. 9-33.
Carey C.C., Strahle J.T., Selinger D.A. & Chandler V.L.(2004). Mutations in the
palealeurone color 1 regulatory gene of the Zea mays anthocyanin pathway have
distinct
phenotypes
relative
to
the
functionally
similar
TRANSPARENTTESTAGLABRA1 gene in Arabidopsis thaliana. Plant Cell,
16: 450–464. http://dx.doi.org/10.1105/tpc.018796
Cermak R. & Wolffram S. (2006). The potential of flavonoids to influence drug
metabolism and pharmacokinetics by local gastrointestinal mechanisms. Current
Drug Metabolism, 7: 729–744. https://doi.org/10.2174/138920006778520570
Cesarone M. R., Laurora G., Ricci A., Belcaco G. & Pomante P. (1992). A cute
effects of Hydroxiethylrutosides on capillary filtration in normal voulenteers,
patients with various hypotension and in patients with diabetic micro angiopathy.
J. Vas. Disease, 21: 76-80.
Cheel J., Schmeda-Hirschmann G., Jordan M., Theoduloz C., Rodriguez J. A.,
Gerth A. & Wilken D. (2007). Free radical scavenging activity and secondary
metabolites from in vitro cultures of Sanicula graveolens. Zeitschrift-furNaturforschung, 62(7/8): 555-562. https://doi.org/10.1515/znc-2007-7-815
Chen S.X., Lan G.C., Ying Y.W., Jiang Y. & Gen S.Y. (2006). Effects of basic
media and culture conditions on callus growth and flavonoid content of
Cyclocarya paliurus. Journal of Fujian Agriculture and Forestry University.
Natural Science Edition, 35(6): 588-592.
Chen-Ying & Cao-FuLiang. (2007). Leave source from callus induction and
flavonoid content in callus from different tissues of five Ginkgo biloba cultivars.
Journal of Zhejiang Forestry College, 24 (2): 150-155.
Chong T.M., Abdullah M.A., Lai Q.M., Nor A.F.M. & Lajis N.H. (2005).
Effective elicitation factors in Morinda elliptica cell suspension culture. Process
in Biochem. 40: 3397–3405. https://doi.org/10.1016/j.procbio.2004.12.028
Christey M.C. & Braun R.H. (2005). Production of hairy root cultures and
transgenic plants by Agrobacterium rhizogenes-mediated transformation.
Methods Mol Biol., 286: 47-60. https://doi.org/10.1385/1-59259-827-7:047
Cody V., Middleton E., Harborne J.B. & Beretz A. (1988). Plant Flavonoids in
Biology and Medicine. II: Biochemical, Cellular and Medicinal Properties.
Progress in Clinical and Biological Research Eds. (Vol. 280). Alan R. Liss: New
York.
Coe E.H. & Neuffer M.G. (1988). The genetics of corn, in Corn and Corn
Improvement, eds G. F. Sprague and J. W. Dudley (Madison, WI: American
Society of Agronomy, 181–258. https://doi.org/10.2134/agronmonogr18.3ed.c3
Collin H.A. (2001). Secondary product formativ in plant tissue cultures. Plant
Growth Regul., 34: 119–34. https://doi.org/10.1023/a:1013374417961
Commenges D., Scotet V., Renaud S., Jacqmin-Gadda H., Barberger-Gateau P.
& Dartigues, J.F. (2000). Intake of flavonoids and risk of dementia. The
European
Journal
of
Epidemiology,
16(4):
357–363.
https://doi.org/10.1023/a:1007614613771
Craig W. J. (1999). Health-promoting properties of common herbs. The American
Journal of Clinical Nutrition, 70(3): 491–499.
Crane C., Wright E., Dixon R., & Wang Z. (2006). Transgenic Medicago
truncatula plants obtained from Agrobacterium tumefaciens-transformed roots
and Agrobacterium rhizogenes-transformed hairy roots. Planta, 223: 1344–1354.
https://doi.org/10.1007/s00425-006-0268-2
Delle Monache G., De Rosa M.C., Scurria R., Vitali A., Cuteri A., Monacelli B.,
Pasqua G. & Botta B. (1995). Comparison between metabolite productions in cell
culture and in whole plant of Maclura pomifera. Phytochemistry, 39(3): 575-580.
https://doi.org/10.1016/0031-9422(94)00971-u
Devi B.P., Vimala, A., Sai, I. & Chandra, S. (2008). Effect of cyanobacterial
elicitor on neem cell suspension cultures. Indian Journal of Science and
Technology, 1:(7).
Dias A.C.P., Tomás-Barberán F.A., Fernandes- Ferreira M. & Ferreres F. (1998).
Unusual flavonoids produced by callus of Hypericum perforatum.
Phytochemistry, 48: 1165–1168. https://doi.org/10.1016/s0031-9422(97)00963-1
Dixon R.A. (2001). Natural products and plant disease resistance. Nature, 411:
843–847. https://doi.org/10.1038/35081178
Dixon R.A., Dey P.M. & Lamb C.J. (1983). Phytoalexins: enzymology and
molecular biology. Advances in Enzymology and Related Areas of Molecular
Biology, 55:1–136. https://doi.org/10.1002/9780470123010.ch1
Dixon R.A., Harrison M.J. & Paiva N.L. (1995). The isoflavonoid phytoalexin
pathway: from enzymes to genes to transcription factors. Plant Physiology, 93:
385-392. https://doi.org/10.1111/j.1399-3054.1995.tb02243.x
Dooner H.K. Robbins T.P. & Jorgensen R.A. (1991). Genetic and developmental
control of anthocyanin biosynthesis. Annu. Rev. Genet., 25: 173–199.
https://doi.org/10.1146/annurev.ge.25.120191.001133
Dornenburg H. & Knorr D. (1995). Strategies for the improvement of secondary
metabolite production in plant cell cultures. Enzyme and Microbial Technology,
17: 674- 684. https://doi.org/10.1016/0141-0229(94)00108-4
Du F., Zhang F. Chen F., Wang A., Wang Q., Yin X. & Wang S. (2011).
Advances inmicrobial heterologous production of flavonoids. African Journal of
Microbiology Research, 5(18): 2566–2574. https://doi.org/10.5897/ajmr11.394
Eguchi K. & Sato T. (2009). Differences in the ratios of cyaniding-3-O-rutinoside
to total anthocyanin under UV and non-UV conditions in tartary buckwheat
(Fagopyrum
tataricum Garten.). Plant
http://dx.doi.org/10.1626/pps.12.150
Prod.
Sci., 12:
150–155.
Ekiert H., Kwiecień I. & Szopa A. (2013). Rosmarinic acid production in plant in
vitro cultures. Pol. J. Cosmetol, 16: 49–58.
Ekiert H., Piekoszewska A., Muszyńska B. & Baczyńska S. (2014).
Accumulation of p-coumaric acid and other bioactive phenolic acids in in
vitro culture of Ruta graveolens ssp divaricata (Tenore) Gams. Med. Int. Rev., 26:
24–31
Ekiert H., Szewczyk A. & Kuś A. (2009). Free phenolic acids in Ruta
graveolens L. in vitro culture. Pharmazie, 64: 100–102
Fakruddin M.D., Hossain Z. & Afroz H. (2012). Prospects and applications of
nanobiotechnology: a medical perspective. J. Nanobiotechnol., 10: 1–8.
https://doi.org/10.1186/1477-3155-10-31
Falcone Ferreyra M.L., Casas M.I., Questa J., Herrera L., Deblasio S., Wang J.,
Jackson D., Grotewold E. & Casati P. (2012). Evolution and expression of
tandem duplicated maize flavonol synthase genes. Front. Plant Sci., 3: 101 .
https://doi.org/10.3389/fpls.2012.00101
Falcone Ferreyra M.L., Rius S.P., & Casati P. (2012). Flavonoids: biosynthesis,
biological functions, and biotechnological applications. Front. Plant Sci., 3: 222.
https://doi.org/10.3389/fpls.2012.00222
Farmer E.E. & Ryan C.A. (1990). Interplant communication-airborne methyl
jasmonate induces synthesis of proteinase inhibitors in plant leaves. Proceedings
of
the
National
Academy
Science,
87:
7713–7716.
https://doi.org/10.1073/pnas.87.19.7713
Fedoreyev S.A., Pokushalova T.V., Veselova M.V., Glebko L.I., Kulesh N.I.,
Muzarok T.I., Seletskaya L.D., Bulgakov V.P. & Zhuravlev Y.N. (2000).
Isoflavonoid production by callus cultures of Maackia amurensis. Fitoterapia,
71: 365–372. https://doi.org/10.1016/S0367-326X(00)00129-5
Feller A., Machemer K., Braun E.L. & Grotewold E. (2011). Evolutionary and
comparative analysis of MYB and bHLH plant transcription factors. Plant J., 66:
94–116. https://doi.org/10.1111/j.1365-313x.2010.04459.x
Ferrer J., Austin, M., Stewart, C.J., & Noel, J. (2008). Structure and function of
enzymes involved in the biosynthesis of phenyl propanoids. Plant Physiol.
Biochem., 46: 356–370. https://doi.org/10.1016/j.plaphy.2007.12.009
Forkmann, G. (1992). Groupe Polyphenols, Lisbon, In Proc. 16th Int. Conf vol.,
16: 19–27.
Fu C.X., Xu Y.J., Zhao D.X. & Ma F.S. (2006). A comparison between hairy
root cultures and wild plants of Saussurea involucrata in phenylpropanoid
production. Plant Cell Rep., 24: 750–754. https://doi.org/10.1007/s00299-0050049-6
Fuhrman B., Buch S. & Vaya J. (1997). Licorice extract and its major polyphenol
glabridin protect low-density lipoprotein against lipid peroxidation: in vitro and
ex vivo studies in humans and in atherosclerotic apolipoprotein E-deficient mice.
The American Journal of Clinical Nutrition, 66(2): 267–275.
464
J Microbiol Biotech Food Sci / Alia Amer 2018 : 7 (5) 457-468
Galway M.E., Masucci J.D., Lloyd A.M., Walbot V., Davis R.W., & Schiefelbein
J.W. (1994). The TTG gene is required to specify epidermal cell fate and cell
patterning in the Arabidopsis root. Dev. Biol., 166: 740–754.
https://doi.org/10.1006/dbio.1994.1352
Georgiev M.I., Pavlov A.I. & Bley T. (2007). Mini Review of Hairy root type
plant in vitro systems as sources of bioactive substances. Appl. Microbiol.
Biotechnol.,74: 1175-1185. https://doi.org/10.1007/s00253-007-0856-5
Ghanati F. & Bakhtiarian S. (2014). Effect of methyl jasmonate and silver
nanoparticles on production of secondary metabolites by Calendula officinalis L.
(Asteraceae). Trop. J. Pharmaceut. Res., 13 (11): 1783–1789.
http://dx.doi.org/10.4314/tjpr.v13i11.2
Ghasemi B., Hosseini R. & Nayeri F.D. (2015). Effects of cobalt nanoparticles on
artemisinin production and gene expression in Artemisia annua. Turk. J. Bot., 39:
769–777. https://doi.org/10.3906/bot-1410-9
Ghoulami S., Idrissi A. I. & Fkih-Tetouani S. (2001). Phytochemical study of
Mentha
longifolia
of
Morocco.
Fitoterapia,
72(5):
596–598.
https://doi.org/10.1016/S0367-326X(01)00279-9
Gil-Izquierdo A., Gil M.I., Ferreres F. & Tom´as- Barber´an F.A. (2001). In vitro
availability of flavonoids and other phenolics in orange juice. Journal of
Agricultural
and
Food
Chemistry,
49(2):
1035–1041.
https://doi.org/10.1021/jf0000528
Giri A. & Narasu M.L. (2000). Transgenic hairy roots: recent trends and
applications. Boitechnol Adv., 18: 1-22. https://doi.org/10.1016/S07349750(99)00016-6
Gomez C., Conejero G., Torregrosa L., Cheynier V., Terrier N. and Ageorges A.
(2011). In vivo grapevine anthocyanin transport involves vesicle-mediated
trafficking and the contribution of antho MATE transporters and GST. Plant J.,
67: 960–970. https://doi.org/10.1111/j.1365-313x.2011.04648.x
Goodman C.D., Casati P., & Walbot V. (2004). A multidrug resistanceassociated protein involved in anthocyanin transport in Zea mays. Plant Cell, 16:
1812–1826. https://doi.org/10.1105/tpc.022574
Grotewold E. (2005). Plant metabolic diversity: a regulatory perspective. Trends
Plant Sci., 10: 57–62. https://doi.org/10.1016/j.tplants.2004.12.009
Grotewold E. (2006). The Science of Flavonoids. Springer: New York, NY.
https://doi.org/10.1007/0-387-28822-8
Grotewold E. & Davis K. (2008). Trafficking and sequestration of anthocyanins.
Nat. Prod .Comm., 3: 1251–1258.
Gupta K. K., Taneja S.C., Dhar K.L. & Atal C.K. (1983). Flavonoids of
Andrographis
paniculata.
Phytochemistry,
22(1):
314–315.
https://doi.org/10.1016/s0031-9422(00)80122-3
Hara Y., Luo S.J., Wickremasinghe R.L. & Yamanishi T. (1995). Special issue
on
tea.
Food
Reviews
International,
11:
371–542.
https://doi.org/10.1080/87559129509541057
Harborne J.B. & Williams, C.A. (2000). Advances in flavonoid research since
1992.
Phytochemistry,
55:
481–504.
https://doi.org/10.1016/S00319422(00)00235-1
Havsteen, B. H. (2002). The biochemistry and medical significance of the
flavonoids.
Pharmacology
and
Therapeutics,
96(2-3):
67–202.
https://doi.org/10.1016/S0163-7258(02)00298-X
Heiras-Palazuelos M.J., Ochoa-Lugo M.I., Gutierrez-Dorado R., Lopez
Valenzuela J.A., Mora-Rochin S. & Milan Carrillo J. et al., (2013).
Technological properties, antioxidant activity and total phenolic and flavonoid
content of pigmented chickpea (Cicer arietinum L.) cultivars. Int. J. Food Sci.
Nutr., 64: 69–76. https://doi.org/10.3109/09637486.2012.694854
Hermann K. (1976). Review of Flavonols and flavones in food plants. J. Food
Technol., 11: 433–448. https://doi.org/10.1111/j.1365-2621.1976.tb00743.x
Hertog M.G.L., Hollman P.C.H. & Katan M.B. (1992). Content of potentially
anticarcinogenic flavonoids of 28 vegetables and 9 fruits commonly consumed in
the Netherlands. Journal of Agricultural and Food Chemistry, 40(12): 2379–
2383. https://doi.org/10.1021/jf00024a011
Hichri I., Barrieu F., Bogs J., Kappel C., Delrot S. & Lauvergeat V. (2011).
Recent advances in the transcriptional regulation of the flavonoid biosynthetic
pathway. J. Exp. Bot., 62: 2465–2483. https://doi.org/10.1093/jxb/erq442
Hooper L. & Cassidy A.A. (2006). Review of the health care potential of
bioactive compounds. Journal of the Science of Food and Agriculture, 86: 1805–
1813. https://doi.org/10.1002/jsfa.2599
Huang X., Yao J., Zhao Y., Xie D., Jiang X. & Ziqin X. (2016). Efficient Rutin
and Quercetin Biosynthesis through Flavonoids-Related Gene Expression in
Fagopyrum tataricum Gaertn. Hairy Root Cultures with UV-B Irradiation. Front.
Plant Sci., 7: 63. https://doi.org/10.3389/fpls.2016.00063
Hussain M.S., Fareed S., Ansari S., Rahaman M.A., Ahmad I. Z. & Saeed M.
(2012). Current approaches toward production of secondary plant metabolites. J.
Pharm Bioallied Sci., 4(2): 10-20. https://doi.org/10.4103/0975-7406.92725
Ionkova L. (2009). Optimization of flavonoid production in cell cultures
of Astragalus missouriensis Nutt. (Fabaceae). Pharmacogn. Mag. 5(18): 92–97.
Kang S.M., Min J.Y., Kim Y.D., Kang Y.M., Park D.J., Jung H.N., Kim S.W. &
Choi M.S. (2006). Effects of methyl jasmonate and salicylic acid on the
production of bilobalide and ginkgolides in cell cultures of Ginkgo biloba. In
Vitro
Cellular
and
Developmental
Biology,
42:
44-49.
http://dx.doi.org/10.1079/IVP2005719
Kelly E.H., Anthony R.T. & Dennis J.B. (2002). Flavonoid antioxidants:
chemistry, metabolism and structure-activity relationships. Journal of Nutritional
Biochemistry, 13(10): 572–584. http://dx.doi.org/10.1016/S0955-2863(02)002085
Kessmann H., Edwards R., Geno P.W. & Dixon R.A. (1990). Stress Responses in
Alfalfa (Medicago sativa L.) “Constitutive and Elicitor-induced Accumulation of
Isoflavonoid Conjugates in Cell Suspension Cultures”. Plant Physiology, 94:
227-232. https://doi.org/10.1104/pp.94.1.227
Khalil M.M., Shehab G.G., Abeer A.M. & Alia A.A. (2008). Influence of
different plant growth regulators on callus induction and flavonoid contents in
alfalfa (Medicago sativa L.). J. Agric. Sci. Mansoura Univ., 33 (6): 4089- 4103.
Khan M.S., Zaka M., Abbasi B.H., Rahman L.U. & Shah A. (2016). Seed
germination and biochemical profile of Silybum marianum exposed to
monometallic and bimetallic alloy nanoparticles. IET Nanobiotechnol., 1-8.
https://doi.org/10.1049/iet-nbt.2015.0050
Kikowska M., Jaromir B., Aldona K. & Thiem B. (2012). Accumulation of
rosmarinic, chlorogenic and caffeic acids in in vitro cultures of Eryngium
planum L. Acta Physiol. Plant, 34: 2425–2433, https://doi.org/10.1007/s11738012-1011-1
Kim Y.K., Li X., Xu H., Park N.I., Uddin M.R. & Pyon, J.Y. et al. (2009).
Production of phenolic compounds in hairy root culture of tartary buckwheat
(Fagopyrum tataricum Gaertn). J. Crop Sci. Biotechnol., 12: 53–58.
https://doi.org/10.1007/s12892-009-0075-y
Kim Y.K., Xu H., Park W.T., Park N.I., Lee S.Y. & Park S.U. (2010). Genetic
transformation of buckwheat (Fagopyrum esculentum M.) with Agrobacterium
rhizogenes and production of rutin in transformed root cultures. Aust. J. Crop
Sci., 4: 485–490.
Koes R., Verweij W. & Quattrocchio F. (2005). Flavonoids: a colorful model for
the regulation and evolution of biochemical pathways. Trends in Plant Sciences,
10(5): 236–242. https://doi.org/10.1016/j.tplants.2005.03.002
Kogawa K., Kazuma K., Kato N., Noda N. & Suzuki M. (2007). Biosynthesis of
malonylated flavonoid glycosides on basis of malonyl transferase activity in the
petals of Clitoria ternatea. Journal of Plant Physiology, 164(7): 886–894.
https://doi.org/10.1016/j.jplph.2006.05.006
Kokotkiewicz A., Bucinski A. & Luczkiewicz M. (2014). Xanthone,
benzophenone and bioflavonoid accumulation in Cyclopia genistoides (L.) Vent.
(honeybush) shoot cultures grown on membrane rafts and in a temporary
immersion system. Plant Cell Tissue Organ Cult., 120(1): 373–378.
https://doi.org/10.1007/s11240-014-0586-1
Kreft S., Knapp M. & Kreft I. (1999). Extraction of rutin from buckwheat
(Fagopyrum esculentum Moench) seeds and determination by capillary
electrophoresis. Journal of Agricultural and Food Chemistry, 47(11): 4649–
4652. https://doi.org/10.1021/jf990186p
Kreft S., Strukelj B., Gaberscik A. & Kreft I. (2002). Rutin in buckwheat herbs
grown at different UV-B radiation levels: comparison of two UV
spectrophotometric and an HPLC method. J. Exp. Bot., 53: 1801–1804.
https://doi.org/10.1093/jxb/erf032
Krolicka A., Szpitter A., Gilgenast E., Romanik G., Kaminski M. & Lojkowska
E. (2008). Stimulation of antibacterial naphthoquinones and flavonoids
accumulation in carnivorous plants grown in vitro by addition of elicitors.
Enzyme
Microb.
Technol.,
42(3):
216–221.
https://doi.org/10.1016/j.enzmictec.2007.09.011
Kuhn B.M., Geisler M., Bigler L. & Ringli C. (2011). Flavonols accumulate a
symmetrically and affect auxin transport in Arabidopsis. Plant Physiol., 156:
585–595. https://doi.org/10.1104/pp.111.175976
Kumar S. & Pandey A.K. (2012). Antioxidant, lipo-protective and antibacterial
activities of phytoconstituents present in Solanum xanthocarpum root.
International Review of Biophysical Chemistry, 3(3): 42–47.
Kumar S., Sharma U.K., Sharma A.K. & Pandey A.K. (2012). Protective efficacy
of Solanum xanthocarpum root extracts against free radical damage:
phytochemical analysis and antioxidant effect. Cellular and Molecular Biology,
58(1): 171–178.
Kunhan J. (1976). The flavonoids: A class of semi-essential food components:
their role in human nutrition. World Res. Nut. Diet., 24:117-119.
https://doi.org/10.1159/000399407
Kutchan T.M. (2005). A role for intra and intercellular translocation in natural
product
biosynthesis.
Curr.
Opin.
Plant
Biol.,
8:
292–300.
https://doi.org/10.1016/j.pbi.2005.03.009
L´azaro M.L. (2009). Distribution and biological activities of the flavonoid
luteolin. Mini-Reviews in Medicinal Chemistry, 9(1): 31–59.
Lan W.Z., Yu L.J., Li M.Y. & Qin W.M. (2003). Cell death unlikely contributes
to Taxol production in fungal elicitor induced cell suspension cultures of Taxus
chinensis
W.
Biotechnol.
Lett.,
25:
47-49.
https://doi.org/10.1023/a:1021726030724
Lee S.Y., Cho S.I., Park M.H., Kim Y.K., Choi J.E. & Park S.U. (2007). Growth
and rutin production in hairy root cultures of buckwheat (Fagopyrum esculentum
465
J Microbiol Biotech Food Sci / Alia Amer 2018 : 7 (5) 457-468
M.).
Prep.
Biochem.
Biotechnol.,
37:
239–246.
https://doi.org/10.1080/10826060701386729
Lei W., Shui X., Zhou Y., Tang S. & Sun M. (2011). Effect of praseodymium on
flavonoids production and its biochemical mechanism of Scutellaria viscidula
hairy root in vitro. Pak. J. Bot., 43(5): 2387-2390.
Li J.X., Xue B., Chai Q., Liu Z.X., Zhao A.P. & Chen L.B. (2005).
Antihypertensive effect of total flavonoid fraction of Astragalus complanatus in
hypertensive rats. The Chinese Journal of Physiology, 48(2): 101–106.
Lopez M., Martinez F., Del Valle C., Orte C. & Miro M. (2001). Analysis of
phenolic constituents of biological interest in red wines by high-performance
liquid chromatography. Journal of Chromatography A., 922(1-2): 359–363.
https://doi.org/10.1016/S0021-9673(01)00913-X
Łuczkiewicz M. & Głod D. (2003). Callus cultures of Genista plants— in vitro
material producing high amounts of isoflavones of phytoestrogenic activity. Plant
Sci., 165: 1101–1108. https://doi.org/10.1016/s0168-9452(03)00305-4
Luczkiewicz M., Kokotkiewicz A. & Glod D. (2014). Plant growth regulators
affect biosynthesis and accumulation profile of isoflavone phytoestrogens in
high-productive in vitro cultures of Genista tinctoria. Plant Cell Tiss Organ
Cult., 118: 419–429. https://doi.org/10.1007/s11240-014-0494-4
Madhavi D.L., Bomser J., Smith M.A.L. & Singletary K. (1998). Isolation of
bioactive constituents from Vaccinium myrtillus (bilberry) fruits and cell cultures.
Plant Sci., 131: 95–103. https://doi.org/10.1016/S0168-9452(97)00241-0
Mahomoodally M.F., Gurib-Fakim A. & Subratty A.H. (2005). Antimicrobial
activities and phytochemical profiles of endemic medicinal plants of Mauritius.
Pharmaceutical
Biology,
43(3):
237–242.
http://dx.doi.org/10.1080/13880200590928825
Manach C. & Donovan J.L. (2004). Review of Farmacokinetics and metabolism
of dietary flavonoids in humans. Free Radical Research, 38: 771–785.
https://doi.org/10.1080/10715760410001727858
Marinova D., Ribarova F. & Atanassova M. (2005). Total Phenolics and total
flavonoids in Bulgarian fruits and vegetables. Journal of the University Chemical
Technology and Metallurgy, 40: 255- 260.
Marrs K.A., Alfenito M.R., Lloyd A.M. & Walbot V. (1995). A glutathione Stransferase involved in vacuolar transfer encoded by the maize gene Bronze-2.
Nature, 375: 397–400. https://doi.org/10.1038/375397a0
Martens S., Preuss A. & Matern U. (2010). Multifunctional flavonoid
dioxygenases: flavonols and anthocyanin biosynthesis in Arabidopsis thaliana L.
Phytochemistry,
71:
1040–1049.
https://doi.org/10.1016/j.phytochem.2010.04.016
Mendhulkar V.D., Patade P. & Vakil M. (2016). Elicitation of flavonoids in
Blumea lacera (Burm.f.) DC. cell culture using chemical elicitor, salicylic acid
and biological elicitor, Aspergillus niger. Int. J. Curr. Res. Biosci. Plant Biol.,
3(11): 85-91. http://dx.doi.org/10.20546/ijcrbp.2016.311.013
Miao Z.Q., Wei Z.J. & Yuan Y.J. (2000). Study on the effects of salicylic acid on
taxol biosynthesis. Sheng Wu Gong Cheng Xue Bao, Chinese Journal of
Biotechnology, 16: 509–513.
Middleton E. (1984). The flavonoids. Trends in Pharmacological Sciences, 5:
335–338.
Middleton E.J. (1998). Effect of plant flavonoids on immune and inflammatory
cell function. Advances in Experimental Medicine and Biology, 439: 175–182.
https://doi.org/10.1007/978-1-4615-5335-9_13
Misra P., Shukla P.K., Pramanik K., Gautam S. & Kole C. (2016).
Nanotechnology for Crop Improvement. In Plant Nanotechnology. Kole et al.
(eds.),
Springer
International
Publishing
Switzerland
2016.
https://doi.org/10.1007/978-3-319-42154-4
Miyake Y., Shimoi K., Kumazawa S., Yamamoto K., Kinae N. & Osawa T.
(2000). Identification and antioxidant activity of flavonoid metabolites in plasma
and urine of eriocitrin-treated rats. Journal of Agricultural and Food Chemistry,
48(8): 3217–3224. https://doi.org/10.1021/jf990994g
Mizukami H., Tabira Y. & Ellis B.E. (1993). Methyl jasmonate induced
rosmarinic acid biosynthesis in Lithospermum erythrorhizon cell suspension
cultures. Plant Cell Reports, 12: 706–709. https://doi.org/10.1007/bf00233424
Mo Y., Nagel C. & Taylor L.P. (1992). Biochemical complementation of
chalcone synthase mutants defines a role for flavonols in functional pollen.
Proc.Natl.Acad.Sci.
U.S.A.,
89:
7213–7217.
https://doi.org/10.1073/pnas.89.15.7213
Mocan A., Crișan G., Vlase L., Crișan O., Vodnar D., Raita O., Gheldiu A., Toiu
A. , Oprean R., & Tilea I.(2014). Comparative studies on polyphenolic
composition, antioxidant and antimicrobial activities of Schisandra
chinensis leaves
and
fruits.
Molecules,
19:
15162–15179.
https://doi.org/10.3390/molecules190915162
Mocan A., Zengin G., Crişan G. & Mollica A. (2016). Enzymatic assays and
molecular modeling studies of Schisandra chinensis lignans and phenolics from
fruit and leaf extracts. J. Enzyme Inhib. Med. Chem., 63(66): 1–11.
http://dx.doi.org/10.1080/14756366.2016.1222585
Mocan M., Schafberg G., Crisan S. & Rohn (2016). Determination of lignans and
phenolic components of Schisandra chinensis (Turcz.) Baill. using HPLC-ESIToF-MS and HPLC-online TEAC: Contribution of individual components to
overall antioxidant activity and comparison with traditional antioxidant assays. J.
Funct. Foods., 24: 579–594. https://doi.org/10.1016/j.jff.2016.05.007
Moscatiello R., Baldan B. & Navazio L. (2013). Plant suspension cultures. In:
Frans JM (Ed.). Plant mineral Nutrients Series: Methods Mol Biol, Vol 953, pp
77-93. Humana Press, Springer: pp. 77-93. https://doi.org/10.1007/978-1-62703152-3_5
Murlidhar A.K., Babu S., Sankar T.R., Redenna P.G., Reddy V. & Latha J.
(2010). Antiinflammatory activity of flavonoid fraction isolated from stem bark
of Butea monosperma (Lam): a mechanism based study. International Journal of
Phytopharmacology, 1: 124–132.
Narayana K.R., Reddy M.S., Chaluvadi M.R. & Krishna D.R. (2001).
Bioflavonoids classification, pharmacological, biochemical effects and
therapeutic potential. Indian Journal of Pharmacology, 33(1): 2–16.
Neuffer M.G., Coe E.H. & Wessler S.R. (1997). Mutants of Maize. Cold Spring
Harbor,
New
York:
Cold
Spring
Harbor
Laboratory
Press.
https://doi.org/10.1017/s0016672397229514
Nijveldt R.J., Van Nood E., Van Hoorn D.E.C., Boelens P.G., Van Norren K. &
Van Leeuwen P.A.M. (2001). Flavonoids: a review of probable mechanisms of
action and potential application. Am. J. Clin. Nutr., 74: 418–425.
Oksman-Caldentey K.M. & Inzé D. (2004). Plant cell factories in the postgenomic era: new ways to produce designer secondary metabolites. Trends Plant
Sci., 9 (9): 433-40. https://doi.org/10.1016/j.tplants.2004.07.006
Ono E., Fukuchi-Mizutani M., Nakamura N., Fukui Y., Yonekura- Sakakibara
K., Yamaguchi M., Nakayama T., Tanaka T., Kusumi T. & Tanaka Y. (2006).
Yellow flowers generated by expression of the aurone biosynthetic pathway.
Proc.
Natl.
Acad.
Sci.,
U.
S.
A.,
103:
11075–11080.
https://doi.org/10.1073/pnas.0604246103
Ortuno A., Gomez P., Baidez A., Frias V. & Del Rio J.A. (2006). Citrus sp: a
source of flavonoids of pharmaceutical interest. Potential Health Benefits of
Citrus. ACS Symp. Ser., 936: 175–185. https://doi.org/10.1021/bk-20060936.ch013
Pandey A. K. (2007). Anti-staphylococcal activity of a pan-tropical aggressive
and obnoxious weed Parthenium hysterophorus: an in vitro study. National
Academy Science Letters, 30(11-12): 383–386.
Pasqua G., Monacelli B., Cuteri A., Finocchiaro O., Botta B., Vitali A. &
Monache G. (1991). Cell suspension cultures of Maclura pomifera: optimization
of growth and metabolite production. Journal of Plant Physiology, 139 (2): 249251. https://doi.org/10.1016/S0176-1617(11)80618-8
Patel H. & Krishnamurthy R. (2013). Elicitors in plant tissue culture. J.
Pharmacog Phytochemi., 2(2): 60-65.
Petroni K., & Tonelli C. (2011). Recent advances on the regulation of
anthocyanin synthesis in reproductive organs. Plant Sci., 181: 219–229.
https://doi.org/10.1016/j.plantsci.2011.05.009
Pires N. & Dolan L. (2010). Origin and diversification of basic-helix- loop-helix
proteins
in
plants.
Mol.
Biol.
Evol.,
27:
862–874.
https://doi.org/10.1093/molbev/msp288
Pourcel L., Irani N.G., Lu Y., Riedl K., Schwartz S., & Grotewold E. (2010). The
formation of anthocyanic vacuolar inclusions in Arabidopsis thaliana and
implications for the sequestration of anthocyanin pigments. Mol. Plant, 3: 78–90.
https://doi.org/10.1093/mp/ssp071
Pourmorad, F., Hosseinimehr, S. J. & Shahabimajd, N. (2006). Antioxidant
activity, phenol and flavonoid contents of some selected Iranian medicinal plants.
The African Journal of Biotechnology. 5(11). 1142–1145.
Radman R., Sacz T., Bucke C. & Keshvartz T. (2003). Elicitation of plants and
microbial cell systems. Biotehnol Appl Biochem., 37: 91-102.
https://doi.org/10.1042/ba20020118
Raei M., Angaji S.A., Omidi M. & Khodayari M. (2014). Effect of abiotic
elicitors on tissue culture of Aloe vera. Int. J. Biosci., 5(1): 74–81.
http://dx.doi.org/10.12692/ijb/5.1.74-81
Rajendran L., Suvarnalatha G., Ravishankar G.A., & Venkataraman L.V. (1994).
Enhancement of anthocyanin production in callus cultures of Daucus carota L.
under influence of fungal elicitors. Appl. Microbiol. Biotechnol., 42: 227-231.
https://doi.org/10.1007/bf00902721
Ralston L., & Yu O. (2006). Metabolons involving plant cytochrome P450s.
Phyto chem. Rev., 5: 459–472. https://doi.org/10.1007/s11101-006-9014-4
Rao S.R. & Ravishankar G.A. (2002). Integration of jasmonic acid and light
irradiation for enhancement of anthocyanin biosynthesis in Vitis
vinifera suspension cultures. Plant cell cultures: chemical factories of secondary
metabolites. Biotechnology Advances, 20: 101–153.
Reinli K. & Block G. (1996). Phytoestrogen content of foods: a compendium of
literature
values.
Nutrition
and
Cancer,
26(2):
123–148.
https://doi.org/10.1080/01635589609514470
Rice-Evans C.A., Miller N.J. & Paganga G. (1996). Structure antioxidant activity
relationships of flavonoids and phenolic acids. Free Radical Biology and
Medicine, 20(7): 933– 956. https://doi.org/10.1016/0891-5849(95)02227-9
Rousseff R.L., Martin S.F. & Youtsey C.O. (1987). Quantitative survey of
narirutin, naringin, hesperidin, and neohesperidin in citrus. Journal of
466
J Microbiol Biotech Food Sci / Alia Amer 2018 : 7 (5) 457-468
Agricultural
and
Food
Chemistry,
35(6):
1027–1030.
https://doi.org/10.1021/jf00078a040
Rusak G., Gutzeit H.O. & Ludwig-Mˆuller J. (2002). Effects of structurally
related flavonoids on hsp gene expression in human promyeloid leukaemia cells.
Food Technol. Biotechnol., 40: 267–273.
Saker M.M. & Kawashity S.A. (1998). Tissue culture and flavonoid content of
Nepeta and Plantago species endemic in Egypt. Fitoterapia, 69(4): 358-364.
Sankaranarayanan S., Bama P. & Ramachandran J. et al., (2010). Ethnobotanical
study of medicinal plants used by traditional users in Villupuram district of Tamil
Nadu. India. Journal of Medicinal Plant Research, 4(12): 1089–1101. doi:
10.5897/JMPR09.027
Sannomiya M., Fonseca V.B. & Silva M.A D. et al., (2005). Flavonoids and
antiulcerogenic activity from Byrsonima crassa leaves extracts. Journal of
Ethnopharmacology, 97(1): 1–6. http://dx.doi.org/10.1016/j.jep.2004.09.053
Saslowsky D.E., Warek U. & Winkel B.S. (2005). Nuclear localization of
flavonoid enzymes in Arabidopsis. J. Biol. Chem., 280: 23735–23740.
https://doi.org/10.1074/jbc.m413506200
Shanks J.V. & Morgan J. (1999). Plant hairy root culture. Curr Opin Biotechnol.,
10: 151-155. https://doi.org/10.1016/S0958-1669(99)80026-3
Sharafi E., Nekoei S.M.K., Fotokian M.H., Davoodi D., Mirzaei H.H. &
Hasanloo T. (2013). Improvement of hypericin and hyperforin production using
zinc and iron nano-oxides as elicitors in cell suspension culture of St John’s wort
(Hypericum perforatum L.). J. Med. Plants By-prod., 2: 177–184.
Sharma D.K. (2006). Bioprospecting for drug, research and functional foods for
the prevention of diseases – Role of flavonoids in drug development. J. Sci. Ind.
Res., 65: 391–401. http://hdl.handle.net/123456789/4836
Sharma M., Sharma A., Kumar A. & Basu S.K. (2011). Review of Enhancement
of secondary metabolites in cultured cells through stress stimulus. American J.
Plant Physiol., 6: 50-71. https://doi.org/10.3923/ajpp.2011.50.71
Shih C.H., Chu H., Tang L.K., Sakamoto W., Maekawa M., Chu I.K., Wang M.
& Lo C. (2008). Functional characterization of key structural genes in rice
flavonoid biosynthesis. Planta, 228: 1043–1054. https://doi.org/10.1007/s00425008-0806-1
Smetanska I. (2008). Production of secondary metabolites using plant cell
cultures.
Adv
Biochem
Eng
Biotechnol.,
111:
187–228.
https://doi.org/10.1007/10_2008_103
Srivastava S. & Srivastava A.K. (2007). Hairy root culture for mass production of
high-value secondary metabolites. Crit. Rev. Biotechnol. Pharmacother., 56: 200207. https://doi.org/10.1080/07388550601173918
Stafford H.A. (1990). Flavonoid Metabolism. CRC: Boca Raton, FL, pp. 1–59.
Stafford H.A. (1991). Flavonoid evolution: an enzymic approach. Plant Physiol.,
96: 680–685. http://dx.doi.org/10.1104/pp.96.3.680
Stewart A.J., Bozonnet S., Mullen W., Jenkins G.I., Lean M.E. & Crozier A.
(2000). Occurrence of flavonols in tomatoes and tomato-based products. Journal
of
Agricultural
and
Food
Chemistry,
48(7):
2663–
2669. https://doi.org/10.1021/jf000070p
Stracke R., Jahns O., Keck M., Tohge T., Niehaus K., Fernie A.R., & Weisshaar
B. (2010). Analysis of production of flavonol glycosides- dependent flavonol
glycoside accumulation in Arabidopsis thaliana plants reveals MYB11-,
MYB12-and MYB111-independent flavonol glycoside accumulation. New
Phytol., 188: 985–1000. https://doi.org/10.1111/j.1469-8137.2010.03421.x
Stracke R., Ishihara H., Huep G., Barsch A., Mehrtens F., Niehaus K. &
Weisshaar B. (2007). Differential regulation of closely related R2R3-MYB
transcription factors controls flavonol accumulation in different parts of the
Arabidopsis
thaliana
seedling.
Plant
J.,
50:
660–677.
https://doi.org/10.1111/j.1365-313x.2007.03078.x
Strittmatter C.D., Rivero M., Wagner M., Kade M., Ricco R.A. & Gurni A.A.
(1991). In vivo and in vitro flavonoid production in Lotus tenuis Waldst. et Kit.
Lotus Newsletter. 22: 14-17.
Su W.W. & Lee K.T. (2007). Plant cell and hairy root cultures – Process
characteristics, products, and applications. In: Shang-Tian Y (Ed.). Bioprocessing
for Value-Added Products from Renewable Resources-New Technologies and
Applications, Elsevier: pp. 263-92. https://doi.org/10.1016/B978-0444521149/50011-6
Sun Y., Li H. & Huang J.R. (2012). Arabidopsis TT19 functionsasa carrier to
transport anthocyanin from the cytosol to tonoplasts. Mol. Plant., 5: 387–400.
https://doi.org/10.1093/mp/ssr110
Szabo E., Thelen A. & Petersen M. (1999). Fungal elicitor preparations and
methyl jasmonate enhance rosmarinic acid accumulation in suspension cultures
of
Coleus
blumei.
Plant
Cell
Reports,
18:
484–
489.
https://doi.org/10.1007/s002990050608
Szopa A. & Ekiert H. (2012). In vitro cultures of Schisandra chinensis (Turcz:)
Baill. (Chinese magnolia vine) – a potential biotechnological rich source of
therapeutically important phenolic acids. Appl. Biochem. Biotechnol. 166: 1941–
1948. https://doi.org/10.1007/s12010-012-9622-y
Szopa A. Ekiert R. & Ekiert H. (2017). Current knowledge of Schisandra
chinensis (Turcz.) Baill. (Chinese magnolia vine) as a medicinal plant species: a
review on the bioactive components, pharmacological properties, analytical and
biotechnological
studies.
Phytochem.
Rev.,
16(2):
195-218.
https://doi.org/10.1007/s11101-016-9470-4
Szopa A., Kokotkiewicz A., Marzec-Wróblewska U., Bucinski A., Luczkiewicz
M. & Ekiert H. (2016a). Accumulation of dibenzocyclooctadiene lignans in agar
cultures and in stationary and agitated liquid cultures of Schisandra chinensis
(Turcz.) Baill. Appl. Microbiol. Biotechnol., 100(9): 3965–3977.
https://doi.org/10.1007/s00253-015-7230-9
Szopa A., Kokotkiewicz A., Bednarz M., Luczkiewicz M. &
Ekiert. H.
(2016b). Studies on the accumulation of phenolic acids and flavonoids in
different in vitro culture systems of Schisandra chinensis (Turcz.) Baill. using a
DAD-HPLC
method.
Phytochemistry
Letters,
https://doi.org/10.1016/j.phytol.2016.10.016
Tadhani M., Patel V.H. & Rema S. (2007). In vitro antioxidant activities of
Stevia rebaudiana leaves and callus. Journal of Food Composition and Analysis,
20 (3/4): 323-329. https://doi.org/10.1016/j.jfca.2006.08.004
Tapiero H., Tew K.D., Ba G.N. & Mathe G. (2002). Review of Polyphenols: do
they play a role in the prevention of human pathologies. Biomedicine Pharmaco
therapy, 56: 200–207. https://doi.org/10.1016/s0753-3322(02)00178-6
Taylor, L. P., & Hepler, P. K. (1997). Pollen germination and tube growth. Ann.
Rev.
Plant
Physiol.
Plant
Mol.
Biol.
48:
461–491.
https://doi.org/10.1146/annurev.arplant.48.1.461
Thiem B., Krawczyk A. & Budzianowski J. (2003). Ellagic acid in in
vitro cultures of Rubus chamaemorus L Herba Pol., 49: 3–4
Thiruvengadam M., Praveen N., Kim E., Kim S. & Chung I. (2014). Production
of anthraquinones, phenolic compounds and biological activities from hairy root
cultures of Polygonum multiflorum Thunb. Protoplasma, 251: 555–566.
https://doi.org/10.1007/s00709-013-0554-3
Thwe A.A., Kim J.K., Li X.H., Kim Y.B., Uddin M.R. & Kim S. J. et al., (2013).
Metabolomic analysis and phenylpropanoid biosynthesis in hairy root culture of
tartary
buckwheat
cultivars.
PLoS
ONE
8:e65349.
https://doi.org/10.1371/journal.pone.0065349
Toda K., Kuroiwa H., Senthil K., Shimada N., Aoki T., Ayabe S.I., Shimada S.,
Sakuta M., Miyazaki Y., & Takahashi R. (2012). The soybean F3_H protein is
localized to the tonoplast in the seed coat hilum. Planta 236: 79–89.
https://doi.org/10.1007/s00425-012-1590-5
Tom´as-Barber´an F.A. & Clifford M.N. (2000). Flavanones, chalcones and
dihydrochalcones-nature, occurrence and dietary burden. Journal of the Science
of Food and Agriculture, 80: 1073–1080. https://doi.org/10.1002/(sici)10970010(20000515)80:7<1073::aid-jsfa568>3.0.co;2-b
Travis S.W., Harsh P.B. & Jorge M.V. (2002). Jasmonic acid-induced hypericin
production in cell suspension cultures of Hypericum perforatum L. (St. John’s
wort)
Phytochemistry,
60:
289–293.
https://doi.org/10.1016/S00319422(02)00074-2
Tripoli E.M., Guardia L., Giammanco S., Majo D.D. & Giammanco M. (2007).
Review of Citrus flavonoids: molecular structure, biological activity and
nutritional
properties.
Food
Chemist.,
104(2):
466–479.
https://doi.org/10.1016/j.foodchem.2006.11.054
Tsurunaga Y., Takahashi T., Katsube T., Kudo A., Kuramitsu O. & Ishiwata M.
et al., (2013). Effect of UV-B irradiation on the levels of anthocyanin, rutin and
radical scavenging activity of buckwheat sprouts. Food Chem., 141, 552–556.
https://doi.org/10.1016/j.foodchem.2013.03.032
Tumova L. & Polivkova D. (2006). Effect of AgNO3 on the production of
flavonoids by the culture of Ononis arvensis L in vitro. Ces Slov Farm., 55(4):
186-188.
Tumova L. & Zapalkova L. (2002). Effect of jasminic acid on production of
flavonoids in a culture of Ononis arvensis L. in vitro. Ceska Slov. Farm., 51: 96–
98.
Valenzuela A., Sanhueza J. & Nieto S. (2003). Natural antioxidants in functional
foods: from food safety to health benefits. Grasas Aceites, 54: 295–303.
http://dx.doi.org/10.3989/gya.2003.v54.i3.245
Vanisree M. & Hsin-Sheng T. (2004). Plant cell cultures - an alternative and
efficient source for the production of biologically important secondary
metabolites. International Journal of Applied Science and Engineering, (2)1: 2948.
Veeresham C. & Chitti V. (2013). Therapeutic agents from tissue cultures of
medicinal plants. Nat Prod Chem Res., 1:4. https://doi.org/10.4172/23296836.1000118
Verpoorte R., Contin A., & Memelink J. (2002). Biotechnology for the
production of plant secondary metabolites. Phytochem. Rev., 1: 13–25.
https://doi.org/10.1023/a:1015871916833
Verpoorte R., Heijden V., Hoopen H.J.G. & Memelink J. (1999). “Metabolic
engineering of plant secondary metabolite pathways for the production of fine
chemicals.”
Biotechnol
Letters,
21:
467-479.
https://doi.org/10.1023/a:1005502632053
Walling L.L. (2000). The myriad plant responses to herbivores. Journal of Plant
Growth Regulation, 19. 195–216.
467
J Microbiol Biotech Food Sci / Alia Amer 2018 : 7 (5) 457-468
Wang H.K. (1999). The therapeutic potential of flavonoids. Experimental
Opinion
Investigation
Drugs,
9:
2103–
2119.
https://doi.org/10.1517/13543784.9.9.2103
Wang J., Qian J., Yao L. & Lu Y. (2015). Enhanced production of flavonoids by
methyl jasmonate elicitation in cell suspension culture of Hypericum perforatum.
Bioresources and Bioprocessing, 2:5. https://doi.org/10.1186/s40643-014-00335
Winkel B.S.J. (2004). Metabolic channeling in plants. Annu. Rev. Plant Biol., 55:
85–107. https://doi.org/10.1146/annurev.arplant.55.031903.141714
Winkel-Shirley B. (2001). Flavonoid biosynthesis. A colorful model for genetics,
biochemistry, cell biology, and biotechnology. Plant Physiol., 126: 485–493.
http://dx.doi.org/10.1104/pp.126.2.485
Wollenweber E. & Dietz V.H. (1981). Occurrence and distribution of free
flavonoid aglycones in plants. Phytochemistry, 20(5): 869–932.
https://doi.org/10.1016/0031-9422(81)83001-4
Xue B., Charest P.J., Devantier Y. & Rutledge R.G. (2003). Characterization of
aMYB R2R3 gene from black spruce (Picea mariana) that shares functional
conservation with maize C1. Mol. Genet. Genomics, 270: 78–86.
https://doi.org/10.1007/s00438-003-0898-z
Yamamoto H., Chatani N., Kitayama A. & Tomimori T. (1986). Flavonoid
production in Scutellaria baicalensis callus cultures. Plant Cell, Tissue and
Organ Culture, 5(3): 219-222. https://doi.org/10.1007/bf00040133
Yamamoto H., Kuribayashi H., Seshima Y. & Zhao P. (2004). Metabolism of
administered (2RS)-naringenin in flavonoid producing cultured cells of Sophora
flavescens.
Plant
Biotechnology,
21(5):
355–359.
https://doi.org/10.5511/plantbiotechnology.21.355
Yamamoto H., Yamaguchi M. & Inoue K. (1995). Stimulation of prenylated
flavonone production by mannans and acidic polysaccharides in callus culture of
Sophora flavescens. Phytochemistry, 40: 77–81. https://doi.org/10.1016/00319422(95)00178-a
Yamamoto H., Yamaguchi M. & Inoue K. (1996). Absorption and increase in the
production of prenylated flavanones in Sophora flavescens cell suspension
cultures
by
cork
pieces.
Phytochemistry,
43:
603–608.
https://doi.org/10.1016/0031-9422(96)00321-4
Yan L., Dong J., Jiang Z. & Tang R. (2004). Study on dynamic accumulation of
secondary metabolites in callus of Eucommia ulmoides. Acta Botanica Boreali
Occidentalia Sinica, 24 (11): 2033-2037.
Yao L.H., Jiang Y.M. & Shi J. et al., (2004). Flavonoids in food and their health
benefits. Plant Foods for Human Nutrition, 59(3): 113–122.
https://doi.org/10.1007/s11130-004-0049-7
Yarizade K. & Hosseini, R. (2015). Expression analysis of ADS, DBR2, ALDH1
and SQS genes in Artemisia vulgaris hairy root culture under nano cobalt and
nano zinc elicitation. Ext. J App Sci., 3(3):69–76. http://ejasj.com/wpcontent/uploads/2015/04/69-76.pdf
Yukimune Y., Tabata H., Higashi Y. & Hara Y. (1996). Methyl jasmonateinduced over-production of paclitaxel and baccatin III in taxus cell suspension
cultures. Nat Biotechnol., 14: 1129–1132. https://doi.org/10.1038/nbt0996-1129
Zhang, B., Zheng, L. P., Yi Li, W. & Wen Wang, J. (2013). Stimulation of
artemisinin production in Artemesia annua hairy roots by Ag-SiO2 core shell
nanoparticles.
Curr
Nanosci.
9:
363–370.
https://doi.org/10.2174/1573413711309030012
Zhang C & Jian-Yong W. (2003). Ethylene inhibitors enhance elicitor-induced
paclitaxel production in suspension cultures of Taxus spp. Cells. Enzyme Microb.
Technol., 32:71–77. https://doi.org/10.1007/10_2013_183
Zhang H.C., Liu J.M., Lu H.Y. & Gao S.L. (2009). Enhanced flavonoid
production in hairy root cultures of Glycyrrhiza uralensis Fisch by combining the
over-expression of chalcone isomerase gene with the elicitation treatment. Plant
Cell Rep., 28:1205–1213. https://doi.org/10.1007/s00299-009-0721-3
Zhang W., Curtin C., Kikuchi M. & Franco C. (2002). Integration of jasmonic
acid and light irradiation for enhancement of anthocyanin biosynthesis in Vitis
vinifera
suspension
cultures.
Plant
Sci.,
162:
459–468.
https://doi.org/10.1016/s0168-9452(01)00586-6
Zhang W., Seki M. & Furusaki S. (1997). Effect of temperature and its shift on
growth and anthocyanin production in suspension cultures of strawberry cells.
Plant Sci.,127: 207–214. https://doi.org/10.1016/s0168-9452(97)00124-6
Zhao, J. & Dixon, R. A. (2010). The ‘ins’ and ‘outs’ of flavonoid transport.
Trends Plant Sci., 15: 72–80. https://doi.org/10.1016/j.tplants.2009.11.006
Zhao J.L., Zou L., Zhang C.Q., Li Y.Y., Peng L.X., Xiang D.B. & Zhao G.
(2014a). Efficient production of flavonoids in Fagopyrum tataricum hairy root
cultures with yeast polysaccharide elicitation and medium renewal process.
Pharmacognosy Magazine, 39 (10): 234-240. https://doi.org/10.4103/09731296.137362
Zhao J., Xiang D., Peng L., Liang Z., Wang Y. & Zhao G. (2014b). Enhancement
of rutin production in Fagopyrum tataricum hairy root cultures with its
endophytic fungal elicitors. Prep. Biochem. Biotechnol., 44: 782–794.
http://dx.doi.org/10.1080/10826068.2013.867872
468