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BioMed Research International
Volume 2016, Article ID 2820454, 9 pages
Research Article

Organogenesis and Ultrastructural Features of In Vitro Grown Canna indica L.

Institute of Biological Sciences, Faculty of Science, University of Malaya, 50603 Kuala Lumpur, Malaysia

Received 18 October 2015; Revised 20 December 2015; Accepted 27 December 2015

Academic Editor: Denise Freire

Copyright © 2016 Sharifah Nurashikin Wafa et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.


An efficient protocol for micropropagation of Canna indica L., an economically and pharmaceutically important plant, was standardized using rhizome explants, excised from two-month-old aseptic seedlings. Complete plant regeneration was induced on MS medium supplemented with 3.0 mg/L BAP plus 1.5 mg/L NAA, which produced the highest number of shoots (73.3 ± 0.5%) and roots (86.7 ± 0.4%) after 2 weeks. Furthermore, the optimum media for multiple shoots regeneration were recorded on MS enriched with 7.0 mg/L BAP (33.0 ± 0.5%). Plantlets obtained were transplanted to pots after two months and acclimatized in the greenhouse, with 75% survival. In addition, ultrastructural studies showed that rhizomes of in vitro grown specimens were underdeveloped compared to the in vivo specimens, possibly due to the presence of wide spaces. Meanwhile, the leaves of in vivo specimens had more open stomata compared to in vitro specimens, yet their paracytic stomata structures were similar. Hence, there were no abnormalities or major differences between in vitro regenerants and mother plants.

1. Introduction

Canna indica L. belongs to the family Cannaceae and is a tropical herb grown from rhizomes and seeds, with banana-like leaves and multicolour flowers. The plant can reach a height of 3 meters and their habitat includes shady areas, wet places in forest and savannah, and swampy areas, along rivers or roadsides. Though C. indica are grown primarily as an ornamental, a recent study shows that proteins contained in the water extract from C. indica fresh rhizome have a potent ability to inhibit human immunodeficiency reverse transcriptase (HIV-RT) virus in vitro (93% at 200 μg/mL) [1]. In a different study, leaf samples of C. indica exhibited the strongest anti-HIV 1 activity compared to roots and rhizome due to the presence of plastocyanin [2]. Furthermore, many parts of C. indica were used in traditional medicine as diaphoretic and diuretic in fevers and dropsy, as a demulcent, to stimulate menstruation, treat suppuration, and rheumatism and to regain energy [3]. It has also been studied for its antitumor, cytotoxic activity and antibacterial properties [4, 5]. Apart from its profound medicinal values, rhizomes of C. indica, which are rich in starch, have traditionally been consumed as boiled rhizome and noodles [6] and used to make alcoholic beverages and flour. Meanwhile, the leaf extracts of C. indica showed great potential as botanical molluscicide [7] and the flower extract exhibited abilities as a natural indicator in acid-base titration [8].

Despite its many medicinal values and uses, traditional propagation of C. indica is hindered by its extremely hard seed coat [9] and slow vegetative propagation of rhizome which is also susceptible to viral infection during multiplication [1013]. Furthermore, common practice of asexual propagation through rhizome produces genetic stagnancy and genetic variation limitations in Canna [14]. Plant tissue culture provides a solution whereby the method rapidly micropropagates plants of superior qualities and free from microorganisms in a relatively short time and minimal space using few starting materials. At the same time, having a reliable micropropagation protocol is a preliminary requirement for any genetic manipulation and protoplast fusion in order to improve Canna variety. The first attempt in this regard using intact rhizome of C. indica did not show high morphogenetic potential and the plant produced insufficient endogenous cytokinin to induce buds proliferation [15]. Later, the same author tried to stimulate shoot development or bud formation from meristem tips with little success [16]. Recently, a study managed to obtain complete plantlets from leaves explant of C. indica via indirect regeneration through in vitro callus and somatic embryogenesis [14].

Considering the norm of vegetative propagation for this plant, current study focuses on establishing direct organogenesis and efficient protocol for in vitro regeneration system of C. indica from rhizome explants. Furthermore, plan for future development and commercialization of this plant requires optimum media for induction of multiple shoots. Lastly, as an early detection system for occurrence of somaclonal variation, ultrastructural features of in vivo and in vitro samples from leaves and rhizomes of this species were examined using Field Emission Scanning Electron Microscope (FESEM).

2. Materials and Methods

2.1. Seeds Scarification and Establishment of Sterile Culture

Initially, we attempted culture with leaf and rhizome explants from in vivo conditions; however, we encountered high problems of contamination and browning. To overcome these, we grew plantlets aseptically in the laboratory and used different seed scarification methods to increase the germination rate. Seeds of red flowered C. indica were purchased from TROPILAB, St. Petersburg, Florida, and germinated under in vitro conditions and on garden soil in the green house as control. Aseptic seedlings were obtained by subjecting C. indica seeds to chemical scarification of sulphuric acid (H2SO4) [9]. The process begins with soaking the seeds in distilled water for 1 day to dulcify or soften the seeds. Next, the seeds were soaked in 100% sulphuric acid (H2SO4) for 3 hours, then rinsed several times, and further soaked in distilled water for one day on a shaker table at 1000 rpm. Prior to inoculation in the laminar flow hood, seeds were surface-sterilized with 70% alcohol for 2 min followed by repeated washing with sterile distilled water. Seeds were then germinated on basal Murashige and Skoog (MS) [17] medium supplemented with 3% (w/v) sucrose and 0.25% gellan gum (Gelzan) as solidification agents [18]. Each flask of 20 mL media was inoculated with one seed and germinated seeds were allowed to grow profusely for two months in culture room at °C under a 16-hour photoperiod, before the rhizomes were excised as explants.

2.2. Complete Plantlet Regeneration and Shoot Multiplication

For organogenesis study, the nutrient medium was prepared by combining commercial MS salts (Sigma), 3% (w/v) sucrose, and 0.25% Gelzan as gelling agent. Plant growth regulators (PGRs) were added to the medium prior to adjustment of pH (5.8) and sterilization (autoclaving at 120°C for 20 min). About 20 mL of the media was evenly dispensed into sterilized tubes where one explant was inoculated per tube. Approximately 5 rhizome explants (~1.0 cm2) per aseptic seedlings were excised and cultured in a horizontal position with the cutting side facing the MS medium augmented with combinations of 1.5–3.0 mg/L 6-benzylaminopurine (BAP) with 1.5–4.5 mg/L 2,4-dichlorophenoxyacetic acid (2,4-D), 1.5–3.0 mg/L BAP with 1.5–4.5 mg/L α-naphthalene acetic acid (NAA), and 1.5 mg/L kinetin (KN) with 1.5–4.5 mg/L NAA to observe direct organogenesis into complete plantlet. Meanwhile, multiple shoots were tried to induce using single hormone of BAP (0.5–9.0 mg/L), KN (0.5–9.0 mg/L), NAA (0.5–3.0 mg/L), and Triiodobenzoic acid (TIBA; 0.5, 1.0 mg/L). All chemicals used were of analytical grade (Sigma Chemical Co., USA). Each treatment consists of 30 replicates. The cultures were maintained in the culture room at temperature of °C under a 16-hour photoperiod with a photosynthetic photon flux density of 50 μmol m−2 s−1 provided by cool white fluorescent lamps.

The cultures were observed daily for any contamination and explants suffering from minor contamination will quickly be transferred into new media. Tubes containing fast growing explants will require frequent subculturing into new media or container in order for growing process to continue. Plant responses were observed and recorded for each replicate after 8 weeks. Multiple shoots induced were later excised and cultured on optimum media for complete plant regeneration.

2.3. Acclimatization of Plantlet

After 2 months, complete plantlets with well-developed shoots and roots from media of direct organogenesis were removed from the culture medium, washed gently under running tap water, and transferred to plastic pots containing black (peat) soils under diffuse light conditions [19]. Plantlets were then covered with clear plastic bags (with holes) and placed in the culture room at temperature of °C for 7 days prior to field transfer to the greenhouse. Watering with tap water was done twice a day with maximum volume of 50 mL per session, at early morning and late evening, for the period of 3 months with constant monitoring.

2.4. Statistical Analysis

All data and variables were statistically analyzed using SPSS statistical package version 11 (SPSS Inc., Chicago, III). Values are presented as mean ± SE. One-way ANOVA and Multiple Range Analysis were done on all data using Duncan’s test at .

2.5. Ultrastructural Studies Using Field Emission Scanning Electron Microscope (FESEM)

Fresh rhizomes and leaves (2 months) of in vivo and in vitro C. indica were collected and cleaned prior to excise into small pieces (specimen) to exhibit important parts of the samples to be viewed. The samples were placed on a stub and examined using a JEOL JSM-7001F Field Emission Scanning Electron Microscope (FESEM).

3. Results and Discussion

3.1. Establishment of Aseptic Seedlings

Preliminary experiments showed that C. indica seeds did not germinate satisfactory in the in vitro condition without scarification. Therefore, the black hard seed coat was scarified mechanically and chemically. The best scarification method was soaking of seeds for three hours in sulphuric acid (H2SO4) which produced the highest percentage of successful seeds germination (84.0%  ± 0.4). Similarly, the positive effects of H2SO4 scarification (more than 90.0%) were also reported by other researches for C. indica seeds sown in the in vivo conditions [9]. In regard to these studies, the slight variations in germination percentage between in vivo and in vitro seed germination could be attributed to the variability of sowing medium and the vigorous method of seeds sterilization. Furthermore, differences in seed viability could be caused by nonhomogeneous seed lots due to uneven maturation and differences in seed dormancy levels [20]. Scarification using H2SO4 was also favoured by seeds of tamarind [21] and bladder-senna [22]. The coatless seed commences germination by breaking the quiescence or dormancy. Process of seed development begins with the formation of radicle (growing root) after day 5. This is followed by the coleoptile which encloses the embryonic shoots and then pushes upward to the surface after day 15. Both will resume elongation and promoting multiple roots, hairy roots, and rhizome after day 30. Once elongation process stops, the first leaf emerged. After two months, aseptic seedlings with well-developed roots and leaves started to accumulate in the sterile tube. Seedlings were then ready to be used as source of explants.

3.2. Induction of Shoots, Roots, and Multiple Shoots

Rhizome explants produced new shoots and roots simultaneously after two weeks of inoculation on MS medium supplemented with combinations of BAP plus NAA. However, root and shoot induction varied in different concentrations of the hormones. High frequency of shoots (73.3%) and roots (86.7%) which resulted in complete plantlet regeneration (Figure 1(a)) was observed in MS medium supplemented with 3.0 mg/L BAP plus 1.5 mg/L NAA. The plantlets grew vigorously (Figure 1(b)) and subsequently required subculturing into larger containers (Figure 1(c)). After 3 months, the plantlets were acclimatized on garden soil, first in the culture room for 7 days and later in the greenhouse (Figure 1(d)). Table 1 shows that lower concentration of BAP with higher concentration of NAA only induced high formation of roots, while increasing the concentrations of NAA with optimum concentration of BAP reduced both shoot and root formation. Meanwhile, the combination of KN and NAA was not as effective as the other hormone combinations at promoting shoots and roots development. In contrast, a previous study [15] reported that intact rhizome explants produced shoot buds and regenerated into complete plantlets effectively in media containing a combination of 2 mg/L IAA and 1 mg/L KN. A further study by Kromer and Kukulczanka [16] was also in disagreement with the present study, whereby they preferred combinations of KN, adenine sulphate, and NAA to combinations of BAP plus NAA. The combinations of BAP plus NAA are substantially important in propagation of various ornamental species, whereby at equal concentration, the combination can yield production of callus while at other concentrations it can result in direct regeneration and rhizogenesis [17].

Table 1: The combined effects of hormones on new shoot and root formation of Canna indica L. after 8 weeks.
Figure 1: Different stages of Canna indica L. plantlet development. (a) Complete plant regeneration after 1 month. (b) Vigorous plantlet growth after 2 months. (c) Subcultured plantlet in a larger container. (d) Acclimatized plantlet on garden soil.

The response of rhizome explants to various plant growth regulators used singly, in terms of shoot, root, and multiple shoot formation, is depicted in Table 2. All single hormones tested induced formation of shoots and roots but at different induction levels. According to the table, the percentage of shoot formation increased with the increase of BAP up to the optimum concentration of 5.0 mg/L and later gradually decreased. The pattern was in agreement with previous researchers [14, 23] which observed a less effective formation of shoots with higher concentrations of BAP. The variants in optimum concentration of BAP for regeneration could be attributed to the types of explants used. Regeneration of plantlets from somatic embryos of C. indica only required low concentration of BAP (2.0 mg/L) [14] while, in the present study, rhizome explants required a high concentration of BAP (5.0 mg/L) to induce optimum shoot and root formation. Similarly, rhizome buds of Curcuma manga give the best response of shoot formation in MS medium containing a high concentration of BAP (9.0 mg/L BAP) [24]. In media with KN only at the concentrations tested, the percentage of shoot formation recorded was less than 60%, while inversely, more than 60% root formation was promoted with the gradual increase of its concentration. A low concentration of TIBA (0.5 mg/L) encouraged formation of shoots, while at higher concentration, the formation of shoots declined drastically and only formation of roots was promoted. TIBA is an antiauxin that promotes lateral shoot initiation in shoot tip culture of Canna edulis [18] and indirect regeneration of turmeric from callus [25]. Among the cytokinins used, BAP was found to be the most suitable in promoting cell division, shoot multiplication, and axillary bud formation, while inhibiting root development [26]. However, we observed profuse rooting in all the cases, which may be a general phenomenon for Canna [14] and the members of Zingiberales as similar phenomena were previously reported in ginger [27] and turmeric [28].

Table 2: Effects of single hormone on shoots, multiple shoots, and root formation of Canna indica L. after 8 weeks.

Multiple shoots of C. indica with more than 20.0% induction were successfully obtained in MS media supplemented with the single hormone of BAP (3.0, 5.0, 7.0, and 9.0 mg/L) and KN (9.0 mg/L) (Table 2). The multiple shoots were healthy with normal looking leaves and roots. The highest number of multiple shoots formation with occurrence of five multiple shoots per explant (Figure 2(a)) was recorded in MS medium supplemented with 7.0 mg/L BAP. Furthermore, there were also observations of four and three multiple shoots per explant on MS medium supplemented with 5.0 mg/L BAP (Figure 2(b)) and 6.0 mg/L BAP (Figure 2(c)), respectively. Induction of multiple shoots using a combination of cytokinin and auxin has been reported by many researchers [24, 29, 30] and is considered as an important step for commercial exploitation of a micropropagation protocol. However, the ability of producing multiple shoots with roots using a single hormone (cytokinin) in a tissue culture system is highly desirable, especially in reducing costs for mass production of any species. However, the optimum requirement at propagule proliferation stage differs from species to species. In research involving other species related to C. indica, shoot multiplication of C. aromatic was found to be optimal at 5 mg/L BAP [31] and for C. zedoary, 3 mg/L BAP was reported to be suitable for multiplication [32].

Figure 2: Multiple shoot induction from Canna indica L. rhizome explants, in (a) 7.0 mg/L BAP; (b) 6.0 mg/L BAP; and (c) 5.0 mg/L BAP after 8 weeks.

Acclimatization of plantlets is the crucial phase where plantlets are in transition from in vitro phase to in vivo phase. Plantlets with well-developed shoot and roots were removed from the culture media and transferred to plastic pots containing black (peat) soils. They were maintained for about 7 days under plastic covers to avoid desiccation prior to field transfer to the greenhouse. The gradual transition process from culture container to the greenhouse produced normal plant growth and morphology with plant survival rate as high as 75.0% by minimizing physiological stress on the regenerated plantlets [33]. Similarly, in another study C. indica acclimatized in clay pots containing an autoclaved mixture of soil and sand produced 72.2% survival rate of regenerated plantlets [14]. On the other hand, a simple acclimatization method was preferred for Kaempferia galangal, whereby a survival rate of 80–90% was easily achieved by dismissing the hardening process and simply keeping the plants in 55% shade and watering twice a day [34].

3.3. Ultrastructural Studies

In a tissue culture system, it is important to produce plantlets identical to the parent plants and avoid formation of somaclonal variation. The present study provides the first comparison between rhizome specimens from in vivo and in vitro C. indica under field emission scanning electron microscope (FESEM). Macromorphologically, no morphological abnormalities in tissue culture raised plants were observed when compared to plants grown in field. However, going deeper into rhizome ultrastructural observations, there were minor structural differences, especially at the outer layer of the rhizome (Figures 3(a) and 3(b)). The In vivo specimen (Figure 3(c)) exhibited an absence of void spaces, while void spaces were very apparent in the in vitro specimen (Figure 3(d)). This indicated that the in vitro rhizome was underdeveloped compared to the in vivo rhizome specimen. It could be hypothesized that since the culture medium was providing all the necessary foods and nutrients to the plant, thus the rhizome’s natural function as a storage compartment for food materials such as starch was underutilized. Furthermore, rhizomes of specimens grown in in vitro conditions required a longer time to reach their full developmental stage or maturity, even though both specimens were collected at the same plant age. According to Mahmad et al. [35], in vitro lotus plants (Nelumbo nucifera Gaertn.) grew vigorously and possessed similar physiological characteristics as the mother plant only after 8 months of acclimatization.

Figure 3: Ultrastructural comparison of Canna indica L. rhizome. The outer layer of in vivo rhizome (a) is smoother and well-formed compared to the in vitro rhizome (b). At 70x magnification, there are no conspicuous void spaces in the in vivo rhizome (c) while void spaces were visible in the in vitro rhizome (d).

Stomata distribution and structure were compared between adaxial and abaxial leaf surface of both in vivo and in vitro specimens of C. indica. Figure 4(a) shows that there are an abundance of open stomata detected on the leaf surfaces of in vivo specimens compared to in vitro specimens that are rich in closed stomata (Figure 4(b)). Open stomata distribution was also much more visible on the abaxial surface (Figure 4(c)) compared to the adaxial surface (Figure 4(a)) of in vivo leaves. This is a normal and expected occurrence of leaves from in vivo conditions. Abundance of closed stomata of in vitro leaves on both adaxial (Figure 4(b)) and abaxial (Figure 4(d)) surfaces could be the result of nonfunctional stomata, which was similarly reported in the potato plant [36]. The stomata were probably nonfunctional or failed to mature to a normal functioning state due to prolonged exposure of the plantlets to high relative humidity and low CO2 concentration. The presence of sucrose in the medium and accumulated ethylene in the headspace of the vessel might also have played a role [37]. As a consequence, photosynthesis, transpiration, and uptake of water, nutrients, and CO2 could be suppressed and dark respiration enhanced, resulting in poor growth [38]. However, functioning closed stomata or plantlet with no fully open stomata is a great acclimatization condition for in vitro plantlets whereby, as a consequence, the plantlet will only wilt slightly and the epidermal cells can recover and become turgid quickly after transfer to ex vitro conditions, leading to increased survival rate [39]. The surface view shows that both in vivo (Figure 5(a)) and in vitro (Figure 5(b)) C. indica leaves possess paracytic stomata, characterized by the position of the subsidiary cell which is parallel to the guard cells [40]. It has typical monocot stomata in which the dumbbell-shape guard cells with unevenly thickened walls are dwarfed by the larger subsidiary cells, which are lacking in dicot stomata [41]. Furthermore, the subsidiary cells and the long axes of the stomata lie parallel to each other. The pores of in vivo stomata (Figure 5(c)) are almost three times bigger than the pores of in vitro stomata (Figure 5(d)).

Figure 4: Surface view of stomata distribution of Canna indica L. leaves. More open stomata are detected on the in vivo leaves ((a) adaxial; (c) abaxial) compared to in vitro leaves ((b) adaxial; (d) abaxial).
Figure 5: Ultrastructural comparison of stomata structure of Canna indica L. leaves. Stomata of in vivo (a) and in vitro (b) leaves are paracytic in structure and the pores of in vivo stomata (c) are larger in comparison with the stomata of in vitro leaves (d).

Electron microscopical observations of rhizome and leaves belonging to regenerants from in vitro culture of C. indica present from many points of view a similar structure with those from the native plants, which demonstrates that our experimental in vitro conditions did not induce significant morphological alterations at the ultrastructural level. Direct complete plant regeneration of C. indica was possible using sterile rhizome explants cultured in MS medium supplemented with 3.0 mg/L BAP plus 1.5 mg/L NAA. Meanwhile, multiple shoots were successfully induced in medium with a high concentration of the single hormone BAP (7.0 mg/L BAP). The finding paves the way for future research on biotechnology manipulations and commercialization, especially in producing virus-free plants and synthetic seed of these medicinally important ornamental species. Furthermore, all plantlets were successfully acclimatized to the greenhouse with 75% survival rate.

Conflict of Interests

The authors declare that there is no conflict of interests regarding the publication of this paper.


The authors would like to thank University of Malaya for the postgraduate PPP grant (PV025/2011) and the facilities provided.


  1. W. Woradulayapinij, N. Soonthornchareonnon, and C. Wiwat, “In vitro HIV type 1 reverse transcriptase inhibitory activities of Thai medicinal plants and Canna indica L. rhizomes,” Journal of Ethnopharmacology, vol. 101, no. 1–3, pp. 84–89, 2005. View at Publisher · View at Google Scholar · View at Scopus
  2. A. Thepouyporn, C. Yoosook, W. Chuakul, K. Thirapanmethee, C. Napaswad, and C. Wiwat, “Purification and characterization of anti-HIV-1 protein from Canna indica L. leaves,” Southeast Asian Journal of Tropical Medicine and Public Health, vol. 43, no. 5, pp. 1153–1159, 2012. View at Google Scholar · View at Scopus
  3. J. A. Duke and E. S. Ayensu, Medicinal Plants of China, vol. 1-2, Reference Publications, Algonac, Mich, USA, 1985.
  4. D. Pornsiriprasert, P. Picha, K. Preechanukool et al., “Studies on the antitumor activity of a Thai folkloric remedy: traditional medicinal plants,” Asian Journal of Pharmacy, vol. 6, p. 124, 1986. View at Google Scholar
  5. W. Avirutnant and A. Pongpan, “The antimicrobial activity of some Thai flowers and plants,” The Mahidol University Journal of Pharmaceutical Sciences, vol. 10, no. 3, pp. 81–86, 1983. View at Google Scholar
  6. N. Tanaka, “The utilization of edible Canna plants in southeastern Asia and southern China,” Economic Botany, vol. 58, no. 1, pp. 112–114, 2004. View at Publisher · View at Google Scholar · View at Scopus
  7. G. K. Rogers, “The Zingiberales (Cannaceae, Marantaceae and Zingiberaceae) in the southeastern United States,” Journal of the Arnold Arboretum, vol. 65, pp. 29–39, 1984. View at Google Scholar
  8. N. S. Mahajan, “Use of Canna indica flower extract as a natural indicator in acid base titration,” Journal of Pharmacy Research, vol. 1, no. 1, 2008. View at Google Scholar
  9. S. C. Joshi and S. C. Pant, “Effect of H2SO4 on seed germination and viability of C. indica a medicinal plant,” Journal of American Science, vol. 6, no. 6, pp. 24–26, 2010. View at Google Scholar
  10. T. Hosoki and H. Sasaki, “In vitro propagation of Canna edulis Ker. by longitudinal shoot-split method,” Plant Tissue Culture Letters, vol. 8, no. 3, pp. 175–178, 1991. View at Publisher · View at Google Scholar
  11. M. T. Momol, B. E. L. Lockhart, H. Dankers, and S. Adkins, “Canna yellow mottle virus detected in Canna in Florida,” Online Plant Health Progress, 2004. View at Publisher · View at Google Scholar
  12. W. A. Monger, V. Harju, A. Skelton, S. E. Seal, and R. A. Mumford, “Canna yellow streak virus: a new potyvirus associated with severe streaking symptoms in canna,” Archives of Virology, vol. 152, no. 8, pp. 1527–1530, 2007. View at Publisher · View at Google Scholar · View at Scopus
  13. M. T. Marino, E. Ragozzino, B. E. L. Lockhart, R. Miglino, and D. Alioto, “First report of Canna yellow mottle virus (CaYMV) in Italy and in the Netherlands,” Plant Pathology, vol. 57, no. 2, p. 394, 2008. View at Publisher · View at Google Scholar · View at Scopus
  14. T. Mishra, A. K. Goyal, and A. Sen, “Somatic embryogenesis and genetic fidelity study of the micropropagated medicinal species, Canna indica,” Horticulturae, vol. 1, no. 1, pp. 3–13, 2015. View at Publisher · View at Google Scholar
  15. K. Kromer, “Biological activity of endogenous and influence of exogenous growth regulators on Canna indica regeneration in vitro,” Acta Horticulturae, no. 91, pp. 295–300, 1979. View at Publisher · View at Google Scholar
  16. K. Kromer and K. Kukulczanka, “In vitro cultures of meristem tips of C. indica,” Acta Horticulturae, vol. 167, pp. 279–285, 1985. View at Google Scholar
  17. T. Murashige and F. Skoog, “A revised medium for rapid growth and bio assays with tobacco tissue cultures,” Physiologia Plantarum, vol. 15, no. 3, pp. 473–497, 1962. View at Publisher · View at Google Scholar
  18. T. Sarai and K. Imai, “The influences of growth regulators and culture medium composition on shoot-tip cultures of edible canna,” Environmental Control in Biology, vol. 45, no. 3, pp. 155–163, 2007. View at Publisher · View at Google Scholar · View at Scopus
  19. R. M. Taha and M. Tijan, “An in vitro production and field transfer protocol for Solanum melongena L. plants,” South African Journal of Botany, vol. 68, no. 4, pp. 447–450, 2002. View at Publisher · View at Google Scholar · View at Scopus
  20. R. Usberti and L. Martins, “Sulphuric acid scarification effects on Brachiaria brizantha, B. humidicola and Panicum maximum seed dormancy release,” Revista Brasileira de Sementes, vol. 29, no. 2, pp. 143–147, 2007. View at Publisher · View at Google Scholar · View at Scopus
  21. S. Muhammad and N. A. Amusa, “Effects of sulphuric acid and hot water treatments on seed germination of tamarind (Tamarindus indica L.),” African Journal of Biotechnology, vol. 2, no. 9, pp. 276–279, 2003. View at Google Scholar · View at Scopus
  22. Z. Olmez and A. Gokturk, “Effects of cold stratification, sulphuric acid, submersion in hot and tap water pretreatments in the greenhouse and open field conditions on germination of bladder-Senna (Colutea armena Boiss. and Huet.) seeds,” African Journal of Biotechnology, vol. 8, no. 13, pp. 2973–2977, 2009. View at Google Scholar · View at Scopus
  23. G. Hussey, “In vitro propagation of Gladiolus by precocious axillary shoot formation,” Scientia Horticulturae, vol. 6, no. 4, pp. 287–296, 1977. View at Publisher · View at Google Scholar · View at Scopus
  24. R. Raihana, Q. Z. Faridah, A. A. Julia, A. H. A. Abdelmageed, and M. A. Kadir, “In vitro culture of Curcuma mangga from rhizome bud,” Journal of Medicinal Plant Research, vol. 5, no. 28, pp. 6418–6422, 2011. View at Publisher · View at Google Scholar · View at Scopus
  25. N. D. Salvi, L. George, and S. Eapen, “Plant regeneration from leaf base callus of turmeric and random amplified polymorphic DNA analysis of regenerated plants,” Plant Cell, Tissue and Organ Culture, vol. 66, no. 2, pp. 113–119, 2001. View at Publisher · View at Google Scholar · View at Scopus
  26. P. Glocke, G. Collins, and M. Sedgley, “6-Benzylamino purine stimulates in vitro shoot organogenesis in Eucalyptus erythronema, E. stricklandii and their interspecific hybrids,” Scientia Horticulturae, vol. 109, no. 4, pp. 339–344, 2006. View at Publisher · View at Google Scholar · View at Scopus
  27. K. B. Kambaska and S. Santilata, “Effect of plant growth regulator on micropropagation of ginger (Zingiber officinale Rosc.) cv. Suprava and Suruchi,” Journal of Agricultural Technology, vol. 5, no. 2, pp. 271–280, 2009. View at Google Scholar
  28. R. K. Tyagi, A. Agrawal, C. Mahalakshmi, Z. Hussain, and H. Tyagi, “Low-cost media for in vitro conservation of turmeric (Curcuma longa L.) and genetic stability assessment using RAPD markers,” In Vitro Cellular and Developmental Biology—Plant, vol. 43, no. 1, pp. 51–58, 2007. View at Publisher · View at Google Scholar · View at Scopus
  29. R. Bharalee, A. Das, and M. C. Kalita, “In vitro clonal propagation of Curcuma caesia roxb and Curcuma zedoaria rosc from rhizome bud explants,” Journal of Plant Biochemistry and Biotechnology, vol. 14, no. 1, pp. 61–63, 2005. View at Publisher · View at Google Scholar · View at Scopus
  30. H. Sunitibala, M. Damayanti, and G. J. Sharma, “In vitro propagation and rhizome formation in Curcuma longa Linn.,” Cytobios, vol. 105, pp. 71–82, 2001. View at Google Scholar · View at Scopus
  31. S. Nayak, “In vitro multiplication and microrhizome induction in Curcuma aromatica Salisb,” Plant Growth Regulation, vol. 32, no. 1, pp. 41–47, 2000. View at Publisher · View at Google Scholar · View at Scopus
  32. N. H. Loc, D. T. Duc, T. H. Kwon, and M. S. Yand, “Micropropagation of zedoary (Curcuma zedoaria Roscoe): a valuable medicinal plant,” Plant Cell Tissue and Organ Culture, vol. 81, no. 1, pp. 119–122, 2005. View at Publisher · View at Google Scholar
  33. J. S. Yaacob, S. Azani, H. Elias, S. Abdullah, N. Mahmad, and N. Mohamed, “In vitro regeneration and acclimatization protocols of selected ornamental plants (Agapanthus praecox, Justicia betonica and Celosia cristata),” Sains Malaysiana, vol. 43, no. 5, pp. 715–722, 2014. View at Google Scholar
  34. P. Chirangini, S. K. Sinha, and G. J. Sharma, “In vitro propagation and microrhizome induction in Kaempferia galanga Linn. and K. rotunda Linn.,” Indian Journal of Biotechnology, vol. 4, no. 3, pp. 404–408, 2005. View at Google Scholar · View at Scopus
  35. N. Mahmad, R. Mat Taha, R. Othman, A. Saleh, N. A. Hasbullah, and H. Elias, “Effects of NAA and BAP, double-layered media, and light distance on in vitro regeneration of Nelumbo nucifera Gaertn. (lotus), an aquatic edible plant,” The Scientific World Journal, vol. 2014, Article ID 745148, 8 pages, 2014. View at Publisher · View at Google Scholar · View at Scopus
  36. S. M. A. Zobayed, F. Afreen-Zobayed, C. Kubota, and T. Kozai, “Stomatal characteristics and leaf anatomy of potato plantlets cultured in vitro under photoautotrophic and photomixotrophic conditions,” In Vitro Cellular and Developmental Biology-Plant, vol. 35, no. 3, pp. 183–188, 1999. View at Google Scholar · View at Scopus
  37. T. Kozai, K. Fujiwara, and I. Watanabe, “Fundamental studies on environments in plant tissue culture vessels. (2) Effects of stoppers and vessels on gas exchange rates between inside and outside of vessels closed with stoppers,” Journal of Agricultural Meteorology, vol. 42, no. 2, pp. 119–127, 1986. View at Publisher · View at Google Scholar
  38. B. R. Jeong, K. Fujiwara, and T. Kozai, “Environmental control and photoautotrophic micropropagation,” Horticultural Reviews, vol. 17, pp. 125–171, 1995. View at Google Scholar
  39. S. M. A. Zobayed, F. Afreen, C. Kubota, and T. Kozai, “Water control and survival of Ipomoea batatas grown photoautotrophically under forced ventilation and photomixotrophically under natural ventilation,” Annals of Botany, vol. 86, no. 3, pp. 603–610, 2000. View at Publisher · View at Google Scholar · View at Scopus
  40. A. E. Radford, W. C. Dickson, J. R. Massey, and C. Ritchie Bell, Vascular Plant Systematics, Harper & Row, New York, NY, USA, 1974.
  41. B. G. Bowes and J. D. Mauseth, Plant Structure: A Colour Guide, Manson Publishing, London, UK, 2nd edition, 2008.