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International Journal of Plant Developmental Biology ©2008 Global Science Books
Recent Advances in the Application
of Plant Tissue Culture in Dieffenbachia
Xiuli Shen1* • Michael E. Kane2
1 Citrus Research and Education Center, Institute of Food and Agricultural Sciences, University of Florida, 700 Experiment Station Road, Lake Alfred, FL 33850, USA
2 Department of Environmental Horticulture, Institute of Food and Agricultural Sciences, University of Florida, Gainesville, FL 32611-1067, USA
Corresponding author: * xis300@ufl.edu
ABSTRACT
Plant tissue culture has been shown to be a very important tool for the ornamental foliage plant industry. This is especially true for the
foliage plant genus Dieffenbachia. The application of in vitro culture of Dieffenbachia has the potential to overcome some of the
limitations associated with traditional methods of mass propagation, breeding and genetic manipulation. However, compared to other
species, this approach has been limited in Dieffenbachia due to its recalcitrant nature in vitro. Recent advances in the application of plant
tissue culture methods for the propagation and genetic manipulation of Dieffenbachia varieties are reviewed.
_____________________________________________________________________________________________________________
Keywords: clonal propagation, shoot organogenesis, somaclonal variation
Abbreviations: 2,4-D, 2,4-dichlorophenozyacetic acid; 2iP, N6-(2 – isopentenyl) adenine; BA, 6-benzyladenine; CPPU, N-(2-chloro-4pyridyl)-N-phenylurea); IAA, indole-3-acetic acid; IBA, indole-3-butyric acid; GA3, gibberellic acid; MS, Murashige and Skoog (1962);
NAA, 1-naphthalene acetic acid; SEM, scanning electron microscopy; TDZ, thidiazuron
CONTENTS
DIEFFENBACHIA GENUS......................................................................................................................................................................... 82
Botany ..................................................................................................................................................................................................... 82
Traditional propagation ........................................................................................................................................................................... 83
Traditional breeding................................................................................................................................................................................. 83
APPLICATION OF PLANT TISSUE CULTURE IN DIEFFENBACHIA................................................................................................... 83
Pathogen-eradicated plant production...................................................................................................................................................... 83
Clonal in vitro propagation ...................................................................................................................................................................... 84
Shoot organogenesis ................................................................................................................................................................................ 84
Somatic embryogenesis ........................................................................................................................................................................... 86
Selection of somaclonal variation............................................................................................................................................................ 88
Polyploidy production ............................................................................................................................................................................. 89
Ovule culture ........................................................................................................................................................................................... 90
FUTURE PROSPECTS ............................................................................................................................................................................... 90
REFERENCES............................................................................................................................................................................................. 90
_____________________________________________________________________________________________________________
DIEFFENBACHIA GENUS
Botany
The genus Dieffenbachia (commonly known as dumb cane)
consists of about 30 monocot species contained in the
family Araceae. Native to tropical regions of Central and
South America (Chen et al. 2003b), the genus is comprised
of herbaceous perennial evergreen species with thick stems
bearing alternate leaves (Black 2002). The value of Dieffenbachia lies in its attractive foliar variegation. The leaves are
broad and variegated with white markings or distinctive
patterns with sheathed petioles resulting in a very striking
appearance (Henny and Chen 2003). Dieffenbachia has a
unique floral structure. Flowers are unisexual and contain
only male or female parts consisting of a spadix and spathe.
The spadix is the central fleshy spike, covered with many
small staminate and pistillate flowers. The spathe is a modified bract and envelops the spadix until anthesis. In Dieffenbachia, separate male and female flowers are on the
same plants with male flowers being on the upper one-or
Received: 1 August, 2008. Accepted: 26 November, 2008.
two thirds of spadix and female flowers on the lower onethird. Male flowers do not produce pollen until 2 to 3 days
after the spathe initially opens while female flowers are
only pollen receptive the same day the spathe unfurls. Thus,
self-pollination is prevented in Dieffenbachia by this naturally occurring dichogamy as female flowers mature earlier
than male flowers (Henny 1988). A special method of pollination is required in Dieffenbachia for seed production
and breeding purposes.
Dieffenbachia requires low light levels for growth. For
example, cv. ‘Star Bright’ and cv. ‘Snow Flake’ tolerate
light levels as low as 50 foot candles (Chen et al. 2003b). In
fact, Dieffenbachia grows significantly better in low rather
than high light conditions. Plants maintained in high light
levels may develop a washed-out appearance. As a result,
Dieffenbachia is widely used as ornamental specimens in
interiorscapes. Besides beautifying the environment, Dieffenbachia is also an ornamental plant with the ability to
remove volatile organic compounds from air and thus functions to improve indoor air quality (Liu 2007). Not surprisingly, Dieffenbachia is among the most popular ornamenInvited Review
International Journal of Plant Developmental Biology 2 (2), 82-91 ©2008 Global Science Books
tal foliage plants in the United States, continually ranking in
the top five for annual wholesale value (McConnell et al.
1989; USDA 1999).
Table 1 30 Dieffenbachia cultivars and their origin.
Cultivars
Type
Origin
Bali Hai
Hybrid
Rex x unnamed rex hybrid
Bausei
Hybrid
Maculate x weirii
Corsii
Hybrid
Maculate x wallisii
GoldRush
Hybrid
Victory x Tropic Marianne
Paradise
Hybrid
Marianne x Wilson Delight
Sparkle
Hybrid
20 parents including Wilson
Delight, Perfection, Perfection
compacta
Star Bright
Hybrid
Several parents
Star White
Hybrid
5 crosses of 9 parents
Sterling
Hybrid
Victory x Tropic Marianne
Triumph
Hybrid
4 crosses of 7 different parents
Tropic Breeze
Hybrid
Fourneri x Angustior Lancifolia
Tropic Honey
Hybrid
Victory x Tropic Marianne
Tropic Marianne Hybrid
Unidentified parent
Tropic Rain
Hybrid
Daguensis x amoena
Tropic Star
Hybrid
Perfection x Angustior Lancifolia
Victory
Hybrid
Wilson Delight x Perfection x
AREC V-78
Camille
Sport
Perfection
Honey Dew
Sport
Camille
Parachute
Sport
Paradise
Snowflake
Sport
Tiki
Tike
Sport
Memeria-Corsii
Tropic Alix
Sport
Tropic Snow
Camouflage
Somaclonal variant Panther
Carina
Somaclonal variant Camille
Rebecca
Somclonal variant
Camille
Sarah
Somclonal variant
Camille
Jungle Giant
Wild collection
Panther
unknown
Gold Dust
unknown
Octopus
unknown
Traditional propagation
Dieffenbachia can be propagated by both sexual and asexual methods. Seed propagation is not usually used because
seed set is very poor, viable seed production is low, and germination is erratic. Consequently, propagation by seeds is
only used for breeding purposes. Dieffenbachia can be easily propagated by asexual methods, by tip, cane cuttings
and divisions. It has been reported that cuttings require
extremely long time periods for root initiation and axillary
bud sprouting. Application of the plant growth regulators
GA3 (gibberellic acid), kinetin and IBA (indole-3-butyric
acid) to stem cuttings either by soaking or direct application
to axillary buds enhances propagation (More and Khalatkar
1988). Traditional asexual propagation can require significant labor inputs and result in the spread of pathogens. The
advantage of propagation by cuttings or divisions is that the
plants propagated are largely true-to-type.
Traditional breeding
Progress in breeding of Dieffenbachia has been slow due to
the long breeding cycles and lack of basic information on
breeding methodology. Hybridization has been the most
common and widely used method for producing new cultivars in Dieffenbachia. Since the first hybrid Dieffenbachia
cv. ‘Bausei’, obtained by a cross between Dieffenbachia
picta and Dieffenbachia weirii, was released in 1870 in the
garden of the Royal Horticultural Society of London at
Chiswick (Birdsey 1951), about 100 new cultivars have
been developed. Hybridization requires many crosses and
careful selection. For example, the hybrid Dieffenbachia cv.
‘Triumph’ was selected from four crosses involving seven
different parents; the hybrid Dieffenbachia cv. ‘Star White’
was generated from five crosses involving nine different
parents; while the hybrid Dieffenbachia cv. ‘Victory’ was
obtained from two crosses involving three parents. Naturally occurring dichogamy in this genus also makes this
process very laborious, time consuming and usually requiring about 7-10 years for a new cultivar to be released. The
Dieffenbachia breeding program at Mid-Florida Research
and Education Center at the University of Florida (Apopka,
FL) was initiated in 1976 and a series of important and popular Dieffenbachia hybrids including Dieffenbachia ‘Sparkles’ (Henny 1995a); Dieffenbachia ‘Star Bright’ (Henny
1995b); Dieffenbachia ‘Triumph’ (Henny et al. 1986,
1987a); Dieffenbachia ‘Starry night’ (Henny et al. 1991b);
Dieffenbachia ‘Star White’ (Henny et al. 1991c); Dieffenbachia ‘Sterling’ (Henny 2006a); Dieffenbachia ‘Tropic
Honey’ (Henny 2006b); Dieffenbachia ‘Tropic Star’ (Henny
et al. 1988a, 1988b); Dieffenbachia ‘Victory’ (Henny et al.
1987b, 1991a), have been released from this program.
In addition to hybridization, new cultivars are also selected as a result of spontaneous mutation in Dieffenbachia
cultivars that are prone to sport. For example, Dieffenbachia
cvs. ‘Carina’, ‘Honey Dew’ and ‘Rebecca’ are sports of cv.
‘Camille’; and cv. ‘Camille’ is a sport of cv. ‘Marianne’.
Cultivars ‘Perfection Compacta’ and ‘Marianne’ are sports
of cv. ‘Perfection’ (Chen et al. 2003a).
Introduction of new species collected from the wild or
private collectors is another way for new cultivar development. For instance, Dieffenbachia cv. ‘Imperial’ was discovered in eastern Peru in 1868 (Birdsey 1951). Regardless
of origin, all new Dieffenbachia cultivars are selected for
their distinctive leaf variegation and shape and plant form
which differs from their parents. A summary of 30 Dieffenbachia cultivars and their origin are listed in Table 1.
Given that foliar variegation and color are the primary
attractive characters of Dieffenbachia, an understanding of
genetic basis of leaf variegation patterns is important in
Dieffenbachia breeding. In general, leaf variegation can
have either a cell lineage or non-cell lineage origin. Cells in
individual plant having different genotypes result in cell
lineage variation. While non-cell lineage variation results
from cells in an individual plant possessing the same genotypes but having differential gene expression. Leaf variation
pattern in Dieffenbachia results from non-cell linage and
follow simple Mendelian rules of inheritance (Henny and
Chen 2003). It has been noted that a single dominant gene
(Pv) (pattern of variation) controlled foliar variegation in
the two Dieffenbachia cvs. ‘Perfection’ and ‘Hoffmannil’.
The difference in leaf variation between these two cultivars
was caused by background modifying genes (Henny 1982).
It was also found that a single dominant allele (Pv1) controlled the foliar variegation pattern of Dieffenbachia cv.
‘Camille’. Pv1 was a mutated form of the Pv allele. The
‘Camille’ variegation pattern masks the ‘Perfection’ and
‘Hoffmannil’ pattern in plants carrying both Pv1and Pv
alleles (Henny 1986). A single dominant nuclear gene (Wm)
(white midrib) controlled the inheritance of the white foliar
midrib in three Dieffenbachia cultivars. The gene for white
midrib (Wm) and the gene for foliar pattern of variegation
(Pv) have also been shown to be linked (Henny 1983).
APPLICATION OF PLANT TISSUE CULTURE IN
DIEFFENBACHIA
Plant tissue culture has been shown to be a very useful tool
for both plant propagation and breeding. It can potentially
overcome some limitations encountered when using traditional approaches to Dieffenbachia propagation and breeding
including the efficient production of disease eradicated
plants.
Pathogen-eradicated plant production
Since the early 1980s, in vitro culture has become an important method for the commercial propagation of Dieffenba83
Dieffenbachia tissue culture: a review. Shen and Kane
bachia cultivars are being commercially produced via micropropagation, surprisingly, there are very few publications on
the in vitro propagation of Dieffenbachia. Voyiatzi and
Voyiatzis (1989) were among the first to describe an in vitro
culture Dieffenbachia protocol for true-to-type plant production through axillary shoot production. Shoot-tip and
lateral bud explants excised from stock plants of Dieffenbachia exotica cv. ‘Marianna’ were surface sterilized in aqueous 2.8% sodium hypochlorite for 15 min, rinsed four times
in sterile distilled water and then cultured in Erlenmeyer
flasks containing 40 ml MS basal medium supplemented
with different plant growth regulators. Media were solidified with 0.7% Difco Bacto agar. Factors examined included type and concentration of two cytokinins (kinetin at 0, 1,
2, and 4 mg/l, and 2iP [N6-(2 – isopentenyl) adenine] at 0,
8, 16 and 32 mg/l), the number of recultures (1 to 4) of the
initial basal shoot clump, and culture temperature (15, 20,
27 and 32°C). Basal medium supplementation with 16 mg/l
2iP was most effective in promoting shoot proliferation (6.2
shoots per flask). Shoot production increased with each
successive reculture of the basal clumps at 6 week intervals,
with 5.5 shoots at the 1st subculture, 8 at the 2nd, 14.4 at 3rd
but then decreased to 0 shoot per flask by the 4th subculture.
Shoot production increased with increasing temperature
reaching a maximum of 6.5 shoots per flask at 27°C, then
decreased to about 1.5 shoots per flask at 32°C when cultured on MS medium supplement with 16 mg/l 2iP. Their
study showed that through manipulation of media and culture conditions, the shoot proliferation rate of Dieffenbachia
can be significantly increased.
chia. Establishment of contaminant-free and pathogen-eradicated cultures is the first goal for any in vitro based propagation protocol because contamination is the biggest hindrance for reliable in vitro propagation (Debergh and Maene
1981). Contaminants on the surface of explants taken from
greenhouse or field can be removed by immersion in certain
steriliants, such as ethanol, sodium hypochlorite or HgCL2
for certain time durations. However, bacteria and fungi may
also reside as endophytes in internal tissue (Kunisaki 1977;
Kane 2000a). It is impossible to remove these internal contaminants by surface sterilization. Consequently, alternative
in vitro culture techniques are required to achieve contaminant free plant production. An initial application of tissue
culture for the propagation of Dieffenbachia was to eliminate systemic viral and bacterial pathogens.
Knauss (1976) described a method to produce Dieffenbachia picta cv. ‘Perfection’ plants free of cultivable fungal
and bacterial contaminants. Lateral buds and meristem-tip
explants (1-3 mm in length) were excised from plants grown
in the greenhouse, surface sterilized and then cultured on a
modified MS (Murashige and Skoog 1962) medium. Cultures exhibiting visible contamination were discarded. Cultures showing no sign of contamination were subject to indexing for cultivable contaminants. The indexing procedure
consisted of 3 steps. In the first step, stems from in vitro
grown plants were cut into 0.5–1.0 mm thick sections, then
the cut sections were divided into groups of four and each
section was cultured onto each of four indexing media. The
remaining shoot tips were subcultured on the medium to
promote continued shoot growth for the next indexing step.
After three weeks culture on indexing media, plantlet lines
showing any fungal and bacterial growth in any of the
indexing media were destroyed. In Step 2, newly-developed
shoot stems from subcultured shoot tips in Step 1 were indexed again using the same procedure. In Step 3, only internodes of stems of plantlets showing no sign of fungal and
bacterial growth from Steps 1 and 2 were subject to indexing. Once again, plantlet lines showing fungal and bacterial
growth in Step 3 were destroyed. Among 82 plantlets examined, Knauss (1976) observed that 32 were contaminated
with bacteria and fungi, while 50 plantlet lines tested free of
fungi and bacteria were retained for further propagation.
These lines displayed vigorous growth and branched more
freely in the absence of fungi and bacteria contaminants.
In addition to providing rapid and reliable propagation,
pathogen eradicated plant lines can also serve as a source
for selection of new cultivars. Chase et al. (1981) reported
the release of the new Dieffenbachia cv. ‘Perfection-137B’
as a result of the selection from pathogen eradicated lines of
Dieffenbachia Maculata generated in vitro. They used the
same experimental procedure as developed by Knauss
(1976), and more than two dozen pathogen-free lines were
produced. Plants from these lines were transferred to soil
and maintained under controlled condition. Plants were evaluated carefully for their growth habit and horticultural
traits. Lines exhibiting slow cutting establishment in soil, or
a tendency to produce sports were eliminated because of
their inferior field performance compared to their parents
and unreliable true-to-type plant production. Finally ‘Perfection-137B’ was selected according to its superior appearance and growth performance.
Shoot organogenesis
Besides clonal propagation from pre-existing meristems
(Kane 2000b), plants can also be produced from adventitious shoot meristems induced to form on explants without
pre-existing meristems via the process of shoot organogenesis (Kane et al. 1991). Shoots may form directly on the explant (direct shoot organogenesis) or indirectly on an intermediary callus which forms on the primary explant (indirect
shoot organogensesis). Orlikowska et al. (1995) provided
the first report of shoot organogenesis on cultured leaf petiole explants in Dieffenbachia. However, leaf petioles were
the only responsive explants for indirect shoot organogenesis as induction of callus on leaf blades and root explants
was not possible and the explants died after 3 to 4 weeks
culture. The inductive period for direct shoot organogenesis
in Dieffenbachia was very long, requiring 6 to 8 weeks incubation in the dark for small visible buds to be formed.
MS basal medium supplemented with 1.0 mg/l TDZ (thidiazuron) plus 1.0 mg/l NAA (1-naphthalene acetic acid) or 1.0
mg/l BA (6-benzyladenine) plus 1.0 mg/l 2,4-D (2,4-dichlorophenozyacetic acid) were the most effective plant growth
regulator combinations for shoot formation, with 15.4 and
10.2% petioles forming buds, respectively. The mean number of buds per responsive explant was 45. However, the
specific cultivar used in this study was not stated and results
were only described in the text, without detailed numeric
data.
At the University of Florida, extensive research was
conducted on shoot organogenesis in Dieffenbachia from
2003 to 2008. For the first time, a protocol for indirect
shoot organogenesis in Dieffenbachia cv. ‘Camouflage’ was
established (Shen et al. 2007a). Lateral buds taken from
plants grown in the greenhouse served as the explant source
to initiate in vitro shoot cultures. Lateral buds were sterilized in 1.2% sodium hypochlorite for 10 min, then rinsed 3
times with sterile water, and cultured in baby food jars (4.4
× 7.0 cm2) containing 40 ml of MS medium supplemented
with 80 μM 2iP and 2 μM IAA (indole-3-acetic acid). Cultures were maintained at 22 ± 3°C under a 16-h light photoperiod provided by cool white fluorescent lights. The axillary shoots formed were transferred to the same fresh medium every 8 weeks to increase in vitro stock shoot cultures.
To detect any cultivable contaminants, established cultures
Clonal in vitro propagation
In vitro propagation (micropropagation), in general, is currently being used to commercially produce a large number
of uniform and true-to-type healthy plants on a year-round
basis. There are many factors affecting explant performance
in vitro, including tissue related factors (genotype and explants) and non-tissue related factors (culture media and
conditions). In order to maximize the efficiency of micropropagation of any species conditions to optimize the five
micropropagation stages must be determined for each plant
by manipulating the various culture and environmental factors affecting in vitro growth responses. Although Dieffen84
International Journal of Plant Developmental Biology 2 (2), 82-91 ©2008 Global Science Books
Fig. 1 In vitro regenerated Dieffenbachia
cv. ‘Camouflage’ plants via indirect shoot
organogenesis. (A) Shoots developed from
calli after 8 weeks culture on MS medium
supplemented with 40 μM 2iP and 2 μM
IAA. (B) Plantlets with fully developed
leaves and roots after 8 weeks cultures on
MS medium supplemented with 40 μM 2iP
and 2 μM IAA. (C) Acclimatized plants
grown in the greenhouse for 8 weeks. Scale
bars = 1 cm.
Table 2 Characterization of calli and their shoot regeneration ability in 4 Dieffenbachia cultivars.
Cultivar
Callus structure
Callus color
Growth rate
Camouflage
nodular
green
medium
Camille
nodular
brown
medium
Octopus
friable
light yellow
high
Star Bright
compact
light green
low
Organogenic
yes
yes
no
yes
Regenerative capacity
> 24 months
16 months
no
2 months
friable calli, produced from cv. ‘Octopus’ leaf explants exhibited no shoot regeneration capacity. While green compact calli from cv. ‘Star Bright’, having a very limited capacity for indirect shoot organogenesis, exhibited no capacity
for sustained callus culture as calli lost their shoot regeneration ability after 2 months culture. Calli of cv. ‘Camille’ retained the capacity for shoot regeneration for up to 16
months. ‘Camouflage’ calli retained the capacity for shoot
regeneration after 24-month culture using 8 week subculture intervals (Table 2). The cultivar ‘Camouflage’ also exhibited the highest shoot production capacity with a maximum of 6.7 shoots/callus, followed by 4.4 shoots/callus
from cv. ‘Camille’ and 3.5 shoots/callus from cv. ‘Star
Bright’ (Shen et al. 2008). Consistent with the report of
Orlikowska et al. (1995), we also observed that root explants displayed no capacity for callus induction regardless
of cultivar or plant growth regulator combination. The in
vitro culture procedures for sustained callus culture and
indirect shoot organogenesis in Dieffenbachia are illustrated
in Fig. 2.
Dieffenbachia is a naturally-slow-growing plant and
this characteristic is also manifested during in vitro culture,
probably indicative of a slow cell division rate. Even when
leaf explants, taken from in vitro produced plants, were
cultured on callus induction media, they responded slowly.
At least 4 weeks culture was required for the first sign of
callus production to be observed. The slow response of leaf
tissue explants in vitro might also be attributed to the need
for a rejuvenation period. It has been noticed that juvenile
tissues responded more quickly than mature tissues when
cultured in vitro (Greenwood 1987; Webster and Jones
1989).
The developmental sequence of indirect shoot organogenesis in Dieffenbachia was investigated using light microscopy. Calli were observed from leaf explants on MS
medium supplemented with 5 μM TDZ and 1 μM 2,4-D
after 28 days of culture. Two types of cells were observed in
calli: 1) regenerative cells which were smaller in size and
more compact with more densely stained cytoplasm, thinner
cell walls, more prominent nuclei and no visible vacuoles
(Fig. 3A); and 2) non-regenerative cells which were larger
and not as compact with less cytoplasm and smaller nuclei,
thicker cell walls and larger vacuoles (Fig. 3B). Early mitotic activity was observed after 31days culture (Fig. 3C).
The first cell division was usually anticlinal followed by
were routinely indexed using the procedure developed by
Kane (2000a). Leaf explants excised from these in vitro
shoot cultures were cultured on the MS medium supplemented with TDZ at 0, 1, 5, 10 μM and 2,4-D at 0, 0.5
and 1 μM for callus induction, initially in dark for 8 weeks
and then transferred to the 16-h light photoperiod for another 4 weeks. The type and concentration of plant growth
regulators had a significant effect on callus induction and
shoot differentiation. The greatest frequency of callus formation (96%) was obtained on medium supplemented with
5 μM TDZ and 1 μM 2, 4-D.
An adventitious shoot regeneration medium was selected by transferring calli onto MS medium supplemented
with 2iP at 0, 20, 40, or 80 μM and IAA at 0 or 2 μM and
then assessing indirect shoot organogenesis after 8 weeks
culture (Fig. 1A). A maximum of 7.9 shoots/callus were
produced on the medium supplemented with 40 μM 2iP and
2 μM IAA. Roots formed spontaneously with shoot formation in most of the Dieffenbachia cultures (Fig. 1B). Shoots
(some with roots) longer than 20 mm with 2-3 leaves were
easily acclimatized to greenhouse conditions after transplanted in plug trays containing a 2:1:1 (v/v/v) mixture of
Canadian peat: vermiculite: perlite. Plantlets were maintained under shade cloth with a maximum irradiance of 345
μmol m-2 s-1, natural photoperiod (10-14.5 h light), and a
temperature range 20-31°C. An ex vitro survival rate of
100% was obtained (Fig. 1C).
The capacity for indirect shoot organogenesis in three
other Dieffenbachia cvs. ‘Camile’, ‘Octopus’ and ‘Star
Bright’ were also examined (Shen et al. 2008). Results indicated that the capacity for indirect shoot organogenesis was
clearly genotype-dependent. Using the same experimental
procedure developed for Dieffenbachia cv. ‘Camouflage’,
we observed distinct differences in callus morphology, callus forming ability, and subsequent shoot differentiation
among the three additional Dieffenbachia cultivars examined. Callus formation frequencies of 96, 62, 54 and 52%
were obtained from cvs. ‘Camouflage’, ‘Camille’, ‘Octopus’ and ‘Star Bright’, respectively.
Four distinct callus types, varying in structure and color,
green nodular, brown nodular, yellow friable and green
compact calli, were produced from cultured leaf explants of
cvs. ‘Camouflage’, ‘Camile’, ‘Octopus’ and ‘Star Bright’,
respectively (Table 2). These different callus types displayed different potentials for shoot organogenesis. Yellow
85
Dieffenbachia tissue culture: a review. Shen and Kane
Stock plants
maintained in a greenhouse
a maximum irradiance: 345 μmol m-2 s-1
natural photoperiod: 10-14.5 h light
temperature range: 20-31° C
1st callus subculture
about 5 mm3 callus pieces
MS + 5 μM TDZ + 1 μM 2,4-D
light intensity: 40 μmol m-2 s-1
photoperiod: 16 h light
temperature: 22° C
Subculture: every 8 weeks
Establishment of in vitro shoot culture
lateral buds explants from stock plants
MS + 80 μM 2iP + 2 μM IAA
light intensity: 40 μmol m-2 s-1
photoperiod: 16 h light
temperature: 22° C
Callus induction
leaf explants from in vitro shoot culture
MS + 5 μM TDZ + 1 μM 2,4-D
light intensity: 40 μmol m-2 s-1
photoperiod: 16 h light
temperature: 22° C
2nd callus subculture
about 5 mm3 callus pieces
MS + 5 μM TDZ + 1 μM 2,4-D
light intensity: 40 μmol m-2 s-1
photoperiod: 16 h light
temperature: 22° C
Subculture: every 8 weeks
Shoot differentiation
about 5 mm3 callus pieces
MS + 40 μM 2iP + 2 μM IAA
light intensity: 40 μmol m-2 s-1
photoperiod: 16 h light
temperature: 22° C
3rd callus subculture
about 5 mm3 callus pieces
MS + 5 μM TDZ + 1 μM 2,4-D
light intensity: 40 μmol m-2 s-1
photoperiod: 16 h light
temperature: 22° C
Subculture: every 8 weeks
Acclimatization and selection of
somaclonal variants
Plantlets > 20 mm with 2 or 3 leaves
Canadian peat: vermiculite: perlite (2:1:1)
a maximum irradiance: 345 μmol m-2 s-1
natural photoperiod: 10-14.5 h light
temperature range: 20-31° C
Sustained callus culture
Fig. 2 Indirect shoot organogenesis and sustained callus subculture for continued shoot production for selection of somaclonal variants.
Hu et al. (2005) reported only meristemoids formed in
superficial cell layers could develop into plants while those
developed from inner cell layers of calli mostly developed
into abnormal adventitious shoots meristems due to the
structural restriction from peripheral cells. Differences in
the species used in these two studies may explain this variation.
We have observed that starch content generally was
lower in cells undergoing intense mitotic activity. Starch
content could be an indicator of the degree of cell differentiation. A cell degeneration process also occurred in some
cells characterized by initial expansion, loss of cytoplasm
and formation of large intercellular spaces. Cell degeneration results in tissue shrinkage and necrosis in other species
(Benelli et al. 2001; Quiroz-Figueroa et al. 2002).
periclinal cell division (Fig. 3D). After several mitotic
division, the differentiation of a meristematic zone occurred
(Fig. 3E). By continuous anticlinal and periclinal cell division, bigger meristematic cell masses composed of actively
dividing cells were formed by 43 days culture. Each meristematic mass was characterized by cells with thick walls
(Fig. 3F). Meristematic cell masses may also develop into
globular shapes, assuming an appearance similar to globular
somatic embryos (Fig. 3G, 3H). Cell divisions usually were
initiated from superficial callus cells (Fig. 3D), but a cell or
a group of cells within the callus may also give rise to a
meristematic mass (Fig. 3I). The meristematic mass became
progressively more organized forming a meristematic dome
which developed into a shoot apical meristem after 12 days
culture on shoot induction medium (Fig. 3J). Cell divisions
along the flanks of the apical meristem resulted in leaf
primordia formation after 18 days following shoot induction
(Fig. 3K). A well-developed adventitious bud with apical
shoot meristem and leaf primordia were formed after 27
days culture (Fig. 3L). Multiple shoots were occasionally
formed (Fig. 3M). Root formation occurred after 39 days of
culture (Fig. 3N). A complete plantlet was regenerated after
8 weeks of culture on shoot induction medium. A vascular
connection between a developing shoot and callus tissue
was detected by day 24 (Fig. 3O). Scanning electron microscopy (SEM) revealed stomata were present on the epidermis of developing leaves by day 36 (Fig. 3P).
The formation of meristemoids was prerequisite for
shoot regeneration which was in agreement with the findings of previous studies in other plants (Choffe et al. 2000;
Budimir 2003). In our study, meristemoids from both surface and internal cells can develop into shoots. However,
Somatic embryogenesis
Somatic embryogenesis is the production of embryos from
somatic cells and not resulting from gametic fusion (Merkle
1997; Von Arnold et al. 2002). Somatic embryos are bipolar,
morphologically and anatomically similar to zygotic embryos and have no vascular connection to the original tissue.
Somatic embryogenesis is known to occur naturally in the
ovule of many plant species and many different terms are
used by different authors to describe this phenomenon in
different species, such as apomixis, polyembryony, adventive, sporophytic and nucellar embryony. Pollen and
many tissues, such as the nucellus, inner integument,
synergids, antipodals, endosperm, and suspensor have been
observed to naturally give rise to asexual embryos (Tisserat
et al. 1979). Given the diverse types of tissues from which
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International Journal of Plant Developmental Biology 2 (2), 82-91 ©2008 Global Science Books
Fig. 3 Histological evidence of indirect shoot organogenesis in Dieffenbachia at different developmental stages when cultured on MS medium
supplemented with 5 μM TDZ and 1 μM 2,4-D for callus induction and on MS medium supplemented with 40 μM 2iP and 2 μM IAA for shoot
differentiation. (A) Regenerative cells in calli originated from leaf explants. Bar = 250 μm. (B) Non-regenerative cells in calli. Bar=250 μm. (C) Early
mitotic activity observed at day 37 on callus induction medium. Bar = 167 μm. (D) Initial anticlinal division on the surface of calli. Bar = 250 μm. (E)
Initiation of meristematic zone by continued anticlinal and periclinal cell division. Bar = 250 μm. (F) Development of meristematic mass by day 43. Bar =
250 μm. (G) Formation of a globular shaped meristematic mass. Bar = 500 μm. (H) Appearance of a globular shaped meristematic mass. Bar = 1 mm. (I)
Meristematic cell mass formed within calli. Bar = 250 μm. (J) Meristematic dome formation after 12 days of culture on shoot differentiation medium. Bar
= 250 μm. (K) Development of shoot meristem and leaf primordia by day 18. Bar = 500 μm. (L) Well-developed shoot bud enclosed by leaves at day 27.
Bar = 500 μm. (M) Multiple shoot formation. Bar = 250 μm. (N) Root formation by day 39. Bar = 250 μm. (O) Vascular connection between a
developing shoot and callus tissue. Bar = 500 μm. (P) SEM depicting a developing shoot with stomata on the leaf epidermis at day 36 culture on shoot
differentiation medium. Bar = 750 μm. (Photos K, N, O from Shen X, Chen J, Kane ME (2007a) Indirect shoot organogenesis from leaves of Dieffenbachia cv.
Camouflage. Plant Cell, Tissue and Organ Culture 89, 83-90, with kind permission of Springer Science + Business Media, ©2007).
embryos can be generated, the more general term nonzygotic embryogenesis has currently been widely adopted.
Somatic embryogenesis can also be induced during in vitro
culture. Since the first report of somatic embryogenesis in
carrot callus cultures in 1958 (Steward et al. 1958a, 1958b),
somatic embryogenesis in vitro has been reported in over
100 species (Merkle and Sommer 1986; Merkle and Wiecko
1989; Merkle et al. 1990; Krishnaraj and Vasil 1995; Merkle et al. 1995). To date, there have been no reports of somatic embryogenesis in Dieffenbachia. Our unsuccessful
attempts to induce somatic embryogenesis, either directly or
indirectly in Dieffenbachia, were partially the results of
high contamination rates (>70%) when culture establishment was attempted using leaf explants taken directly from
greenhouse-grown donor plants. Leaves excised from
greenhouse grown stock plants of Dieffenbachia cvs. ‘Camouflage’ and ‘Camille’ were rinsed in running water for 10
min, and then sterilized in aqueous 1.2% sodium hypochlorite (20%, v/v) for 10 min followed by three 5-min rinses
with sterile water. Leaf explants were then cut into about 5mm2 sections and cultured on induction media for somatic
embryogenesis. Induction media were composed of MS
basal medium supplemented with different concentrations
and combinations of PGRs (plant growth regulators). PGRs
tested were: (1) BA at 0, 1, 10, 50 μM and 2,4-D at 0, 1, 10,
50 μM; (2) CPPU [N-(2-chloro-4-pyridyl)-N-phenylurea] at
0, 1, 2.5, 5 μM and 2,4-D at 0, 2, 4, 8, 10 μM; (3) CPPU at
0, 1, 2.5, 5 μM and NAA at 0, 2, 4, 8, 10 μM ; (4) kinetin at
87
Dieffenbachia tissue culture: a review. Shen and Kane
terminated with formation of meristematic tissues (Bouman
and De Klerk 1997). Compared to natural sport production,
somaclonal variation occurs at a much higher rate. Somaclonal variation can result from either pre-existing variation
in explant tissues or induced variation during tissue culture
(Skirvin et al. 1994).
In addition to facilitating clonal propagation, in vitro
culture can also result in production of off-type plants. In
the early application of tissue culture for commercial propagation of Dieffenbachia, all off-type plants were rouged out
to maintain the genetic fidelity of the plants produced. It
was later realized that these off-type plants could be a
source for selection of somaclonal variation for new cultivar development.
Among the factors affecting in vitro regeneration of
somaclonal variants, genotype plays an important role. The
potential for and frequency of somaclonal variation is genotype-dependent (Merkle 1997). During the assessment of
somaclonal variation in Dieffenbachia regenerated through
indirect shoot organogenesis, Shen et al. (2007b) noted that
the rates of somaclonal variation were 40.4 and 2.6% among
regenerated cvs. ‘Camouflage’ and ‘Camille’ plants, respectively. Cultivar ‘Star Bright’ displayed no potential for producing somaclonal variants while all regenerated ‘Star
Bright’ plants were true-to-type. It was also found that duration of callus culture had no effect on somaclonal variation
rates of cv. ‘Camouflage’ as the somaclonal variation rates
between plants regenerated from 8 months and 16 months
of callus culture were similar. This is inconsistent with the
general belief that somaclonal variation increases with the
length of time that a culture has been maintained in vitro.
Orton (1985) noted that if calli, derived from immature
petiole segment, were maintained for 6 months by a series
of repeated subculture transfers, 84% of the callus cells
were karyologically indistinguishable from the control. The
remaining 16% exhibited chromosome loss or fusion with
only 1 regenerated plant out of 95 displaying an abnormal
phenotype. After 12 months in culture, 97% of the callus
cells were karyologically distinguishable from the control.
Most cells were aneuploids and all callus cells lost the capacity to produce embryoids.
Somaclonal variation is often associated with indirect
shoot organogenesis or somatic embryogenesis, each of
which involves an interviewing callus stage. During this period, differentiated cells undergo dedifferentiation, induction, redifferentiation (Rout 1999). Bouman and De Klerk
(2001) showed that the rate of somaclonal variation among
Begonia regenerated via somatic embryogenesis was 1.5%
for direct but 10.6% for regenerants derived from the callus
stage. Since Larkin and Scowcroft (1981) advocated that
somaclonal variation could be used as a promising tool for
breeding to produce novel genetic variation, foliage plant
somaclones with commercially desirable characteristics
have been generated by this method (Chen et al. 2006).
Any change at the phenotypic level, such as foliar
variegation pattern, alterations in leaf shape and texture, or
variation in overall plant form, can be a desirable trait in
Dieffenbachia because the value of Dieffenbachia lies in its
aesthetic appearance (Chen et al. 2003a). Three types of
somaclonal variants with novel and distinct foliar variegation patterns differing from the parental plants have been
obtained in Dieffenbachia ‘Camouflage’ plants regenerated
from leaf-derived calli via indirect shoot organogenesis (Fig.
4). One type of somaclonal variant bearing lanceolate
leaves instead of oblong leaves of the parent has been identified from regenerated cv. ‘Camille’ plants (Fig. 5).
There are two major advantages of indirect shoot organogenesis in vitro. A large number of shoots can be produced from an explant following callus induction and shoot
formation. It also has great potential for regenerating somaclonal variants due to intervening callus phase and resultant
genetic instability. Selection of somaclonal variants from in
vitro cultures has become an important method for new cultivar development since it can hasten the breeding process.
It generally requires from 2 to 3 years to develop a new cul-
0, 1, 5, 10 μM and IAA at 0, 1 μM ; (5) dicamba at 0, 1, 3, 9
μM and 2,4-D at 0, 1 μM; (6) picloram at 0, 1, 3, 9 μM and
2, 4-D at 0, 1 μM; (7) TDZ at 0, 1, 10, 50 μM and NAA at 0,
1, 10, 50 μM; (8) TDZ at 0, 1, 10, 50 μM and 2,4-D at 0, 1,
10, 50 μM; and (9) TDZ at 0, 1, 5, 10 μM and 2,4-D at 0,
0.5, 1 μM. Explants were cultured in 100 × 15 mm sterile
Petri plates containing 20 ml medium. There were 5 explants per Petri plate and 5 replicate plates per treatment.
Cultures were initially maintained in dark for 8 weeks and
then transferred to the 16 h photoperiod for another 4 weeks.
Unfortunately, all PGRs screened failed to induce somatic
embryogenesis (unpublished data).
Dieffenbachia is mainly propagated vegetatively by
cuttings and divisions and is maintained under moist and
shaded condition. Conceivably, under these cultural conditions more bacteria and fungi may accumulate on the surface of plants or even inside plants as endophytes. This may
account for such high contamination rates experienced
when attempting to establish in vitro cultures. Furthermore,
leaf explants, even when not contaminated, were not responsive on any of the media tested. Using leaf explants
from established shoot cultures is an alternative means to
reduce contamination rate and increase explant response.
However this approach has not been attempted.
We have been successful in inducing regeneration of
nodular structures from leaf explants of both cvs. ‘Camouflage’ and ‘Camille’. Morphologically, these nodules resemble somatic embryos. We also found that these nodular
structures were comprised of actively dividing cells. However, the absence of bipolar structure (shoot and root meristems) in more developed nodules indicates that these nodules were not somatic embryos.
The factors and mechanisms determining the capacity
for cellular regenerative as well as the subsequent developmental pathway are largely unknown, but undoubtedly, the
type and concentration of plant growth regulators in the medium play a role in the determination of cell differentiation
(Onay 2000). Ma and Xu (2002) reported that the same
cells may give rise to either somatic embryogenesis or shoot
organogenesis depending on the duration of induction and
plant growth regulators included in media. This suggests
that plant growth regulators could determine the developmental pathway of competent cells. However, attainment of
competence is not clearly understood. The presence of inductive signals, for instance, plant growth regulators in culture medium, was necessary for a cell to become competence (Rugini and Muganu 1998). Compete cells may subsequently form meristematic cells. Meristematic cells may
give rise to the formation of meristemoids. Once meristemoids are produced, some of them may develop into adventitious shoots, roots or somatic embryos. It has also been
demonstrated that the in vitro regeneration pathway could
be shifted by manipulation of plant growth regulators in
culture media in other species. It was possible in some species to switch regeneration from shoot organogenesis to somatic embryogenesis by increasing the TDZ concentration
in the medium. TDZ induced shoot organogenesis at low
concentration (< 2.5 μM) and somatic embryogenesis at
high concentration (5-10 μM) in African violet (Mithila et
al. 2003). In our study we also tried to induce somatic embryogenesis from leaf derived calli of Dieffenbachia by increasing concentration of TDZ from 5 to 10, 20, 40 and 80
μM in media. Unfortunately, there was no evidence for the
occurrence of somatic embryogenesis.
Selection of somaclonal variation
The genetic variation among plants regenerated from in
vitro culture has been termed somaclonal variation (Larkin
and Scowcroft 1981). Plants with the deviant phenotypes
are known as somaclones or somaclonal variants. Somaclonal variation is a random phenomenon that can occur at any
location in the genome (De Schepper et al. 2003). From its
origin, it can be deduced that somaclonal variation occurs in
the period before the formation of meristematic tissues and
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International Journal of Plant Developmental Biology 2 (2), 82-91 ©2008 Global Science Books
Fig. 5 Dieffenbachia cv. ‘Camille’ plants regenerated by indirect shoot
organogenesis showing variation in leaf shape. (A) Parental type plants
with oblong shaped leaves. (B) Somaclonal variants with lanceolate
leaves. Bars = 1 cm. (From Shen X, Chen J, Kane ME (2007b) Assessment of
somaclonal variation in Dieffenbachia plants regenerated through indirect shoot
organogenesis. Plant Cell, Tissue and Organ Culture 91, 21-27, with kind permission
of Springer Science + Business Media, ©2007).
tivar via somaclonal variation compared to 7 to 10 years
using traditional breeding techniques (Henny et al. 2000).
Polyploidy production
Polyploidy occurs naturally in some plant species and can
also be induced in vitro. Since Murashige and Nakano
(1966) first reported the successful induction of polyploidy
in tobacco in vitro, it has been employed as a breeding tool
to overcome sexual sterility (Von Aderkas and Anderson
1993). Production of tetraploids in Dieffenbachia cv. ‘Star
Bright’ was reported by Holm (2007). Cultivar ‘Star Bright
M-1’, a somaclonal variant of cv. ‘Star Bright’, was selected
among the regenerated plants. Cultivar ‘Star Bright M-1’ is
a desirable breeding parent for its unique leaf variegation
pattern and bushy appearance, however, it is sterile. The establishment of in vitro culture of Dieffenbachia ‘Star Bright
M-1’ was achieved by culturing shoot tips on MS medium
supplemented with 2iP at 10 mg/l and IAA at 0.1 mg/l.
Shoot cultures were subcultured at 6 week interval to regenerate sufficient plants for colchicine treatment. Four colchicine concentrations of 0, 250, 500 and 1000 mg/l were
screened. Shoot clumps were soaked in colchicine solution
Fig. 4 Dieffenbachia cv. ‘Camouflage’ plants regenerated by indirect
shoot organogenesis showing variation in leaf variegation and color.
(A) Parental plant: creamy, camouflaged leaves with random green batches of different size. Bar = 1 cm. (B) SV1 (Somaclonal Variation): solid
dark green leaves with whitish variegation along the midvein. Bar = 1 cm.
(C) SV2: light green leaves with many yellowish spots, and connections
among spots resulted in large yellowish blotches. Bar = 1 cm. D) SV3:
green leaves with few scattered yellowish spots. Bar = 1 cm. (From Shen X,
Chen J, Kane ME (2007b) Assessment of somaclonal variation in Dieffenbachia
plants regenerated through indirect shoot organogenesis. Plant Cell, Tissue and
Organ Culture 91, 21-27, with kind permission of Springer Science + Business
Media, ©2007).
89
Dieffenbachia tissue culture: a review. Shen and Kane
for 24 hours on a shaker, then transferred onto the same MS
medium used for shoot culture. Following colchicine treatment, shoot clumps were subcultured at 6-week intervals.
Regenerated shoots, longer than 2 cm, were removed from
the shoot clumps and acclimatized to greenhouse condition
for further evaluation. Among 422 surviving plants following colchicine treatment, 63 plants displayed visible traits of
polyploidy. These polyploid plants were potential candidates as parents for breeding.
to be a powerful tool for plant improvement including phenotypic and production traits of many species (Rego and
Faria 2001). Given the ability to regenerate plants from
callus via shoot organogenesis, there is no doubt that the
application of genetic transformation techniques will prove
beneficial to the genetic improvement of Dieffenbachia in
the future.
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In some species, especially in interspecific and intergeneric
crosses, embryo abortion occurs at an early stage, and difficulties in excising embryo are encountered. Following fertilization ovules were excised and cultured on medium in
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FUTURE PROSPECTS
Somatic embryogenesis has many advantages over shoot
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and root meristems and, as such, the rooting stage can be
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The establishment of a protocol for somatic embryogenesis
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Dieffenbachia is mainly propagated by vegetative
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International Journal of Plant Developmental Biology 2 (2), 82-91 ©2008 Global Science Books
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