Scientifica
Volume 2016 (2016), Article ID 5813851, 7 pages
http://dx.doi.org/10.1155/2016/5813851

Research Article

Micropropagation, Micromorphological Studies, and In Vitro Flowering in Rungia pectinata L.

Mahipal S. Shekhawat, M. Manokari, and C. P. Ravindran

Biotechnology Laboratory, Department of Plant Science, MGGAC, Mahe, Pondicherry 673 311, India

Received 18 December 2015; Accepted 14 April 2016

Academic Editor: Marie-Aleth Lacaille-Dubois

Copyright © 2016 Mahipal S. Shekhawat 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.

Abstract.

A tissue culture protocol was developed for an important medicinal plant Rungia pectinata L. in the present study. Nodal shoots were used as explants and surface-sterilized with 0.1% HgCl₂ solution. Murashige and Skoog (MS) medium was used to establish the cultures of R. pectinata. The bud break was reported on MS medium supplemented with 1.0 mg L⁻¹ 6-benzylaminopurine (BAP). About 98% response was observed with this media combination and maximum 3.2 shoots per explant with 4.3 cm length were recorded. The shoots were further multiplied using MS medium augmented with 0.5 mg L⁻¹ each of BAP and kinetin (Kin) + 0.1 mg L⁻¹ indole-3 acetic acid (IAA). Maximum 13.2 shoots per explant with 5.2 cm length were observed. All the shoots were rooted (4.9 roots per shoot with 3.5 cm length) on half strength MS medium fortified with 2.0 mg L⁻¹ indole-3 butyric acid (IBA). In vitro flowering was induced from the shoots on half strength MS medium supplemented with same concentrations and combinations of growth regulators used for shoot multiplication under 12/12 hr light/dark photoperiod. The plantlets were hardened in the greenhouse for two months and finally transferred to the field. The foliar micromorphological studies revealed the developmental changes in stomata, vein density, and trichomes during the culture of shoots under in vitro conditions.

1. Introduction

Rungia pectinata L. is an ethnomedicinal plant which belongs to the family Acanthaceae. R. parviflora var. pectinata, R. parviflora var. muralis, and Justicia pectinata are the synonyms of this plant. It is an annual erect herb with profuse branching and distributed throughout the warmer parts of India [1]. The herb possesses cylindrical fragile stems which bloom during the months of November-December [2].

Phytosterols, terpenes, tannins, glycosides, flavonoids, phenolic compounds, amino acids, fixed oils, and so forth are important phytochemicals isolated from this plant [3]. The flowers are reported to contain isosalipurposide, luteolin, glucoside, lutein, delphinidin-3,5-diglucoside, and pigments [4]. The juice prepared from the leaves is considered as cooling agent and used to cure smallpox in the infants. Bruised leaves are externally applied to relieve painful inflammations and swellings [5]. The paste prepared from fresh leaves mixed with castor oil is reported to cure tinea capitis, a scaly fungoid infection on scalp. Roots are used as febrifuge and vermifuge by the tribal population in India [6, 7]. R. pectinata have been claimed to exhibit antipyretic, anti-inflammatory, diuretic, analgesic, antifungal, and antimicrobial activities [4, 8, 9].

Recently, due to high demand by the drug manufacturers, this plant has been overexploited. The natural population of R. pectinata is decreasing in the forests. Therefore, conservation activities have been initiated by the Wildlife Institute of India [10].

The transfer of vegetative phase to reproductive phase is a complicated and fascinating process in the life cycle of the plants. Environmental factors, photoperiod, and genetic makeup of the plant are responsible for flowering phenomena [11]. Reproductive phase can be induced by the artificial manipulation of these factors under in vitro controlled environment [12]. In vitro flowering can be induced artificially by altering the concentration of plant growth regulators, different light qualities, photoperiods, and so forth [13–18]. The in vitro approach enables early flowering in the plants and could help in understanding the suitable sites of tissues for the flower induction.

The in vitro growing plants develop inefficient stomata, reduced epicuticular wax, and photosynthetic tissues; these features promote low regulation mechanism of water loss [19]. Therefore, the micropropagated plants failed to survive in the greenhouse and field trials [20]. Distribution and forms of trichomes, stomata, and venation pattern may vary depending on the environmental conditions [21]. The micromorphological studies of leaves could help in understanding the developmental changes in the leaf anatomy when the plants are cultured in the laboratory conditions.

Till date, the bioprospection reports on R. pectinata are restricted to the biological activities and isolation of different chemical compounds only. This is the first report on development of micropropagation protocol as conservation strategy and in vitro flowering in R. pectinata using nodal shoot segments.

2. Materials and Methods

2.1. Plant Material and Culture Initiation

Actively growing young shoots of R. pectinata were harvested from the forest areas of South India. The nodal segments were dissected with two nodes, rinsed in running tap water, and immersed in 2% Tween® 20 detergent solution for 15 min. The explants were then treated with 0.1% (w/v) Bavistin (systemic fungicide, BASF Pvt. Ltd., India) solution for 5 min and washed thoroughly in sterile distilled water. Finally the explants were surface-sterilized using 0.1% (w/v) solution of mercuric chloride for 4-5 min and rinsed with autoclaved distilled water for 5-6 times to remove the traces of sterilant. The sterilized explants were inoculated vertically on culture medium after trimming both the cut ends.

2.2. Culture Medium and Culture Conditions

Murashige and Skoog [22] (MS) medium consists of 30 g L⁻¹ sucrose, 8.0 g L⁻¹ agar, and additives (ascorbic acid 50 mg L⁻¹, citric acid, adenine sulphate, and arginine each 25 mg L⁻¹) which was used to establish the cultures in vitro. pH of the medium was adjusted to 5.8 using 0.1 N NaOH or HCl. Culture vessels with medium were capped using cotton plugs or polycarbonate caps and autoclaved at 121°C and 104 kPa for 15 min. The cultures were initiated using MS medium supplemented with 6-benzylaminopurine (BAP) and kinetin (Kin) ranging from 0.5 to 3.0 mg L⁻¹. The cultures were incubated at °C temperature for the photoperiod of 16 hr with 30 μmol m⁻² s⁻¹ Spectral Flux Photon Density (SFPD) light provided by cool white fluorescent tubes.

2.3. In Vitro Multiplication of Shoots

The explants with fresh shoots from the initiation stage were cut into small nodal segments containing two nodes and subcultured on multiplication medium, augmented with various concentrations and combinations of BAP, Kin (0.0–2.0 mg L⁻¹), and indole-3 acetic acid (IAA, 0.1–0.4 mg L⁻¹). The subculture process was continuously repeated for up to four subcultures (each of four-week duration) to study the effect of subculture duration and growth hormones for stable multiplication of the shoots. The culture observations were recorded and the number and height of shoots were calculated after 4 weeks.

2.4. In Vitro Flowering

To induce flowering in vitro, the healthy shoots from third-fourth subculture stage of multiplication phase were isolated and inoculated to half strength MS medium containing growth hormones as described in multiplication stage and maintained under different photoperiods (12/12 hr/d, 16/8 hr/d, and 8/16 hr/d).

2.5. In Vitro Rooting of Shoots and Hardening of Plantlets

Healthy and mature elongated shoots measuring the size of 3.0–4.0 cm were harvested from the fourth subculture stage of multiplication. These shoots were dissected and transferred to different strengths of MS medium augmented with IAA, indole-3 butyric acid (IBA), and α-naphthalene acetic acid (NAA) individually to study the efficacy of auxins and medium strength in induction of roots in vitro. The entire rooting experiment was kept under diffused light area for a week and then shifted to the photon rich area of the culture room.

After four weeks of incubation, the well-rooted shoots were separated from the culture vessels and thoroughly washed with tap water. The plantlets with healthy roots were transferred to disposable paper cups (Vandana Paper Products, Chennai, India) containing 55 g sterile Soilrite®, moistened with one-fourth MS salts solution, and maintained in high humidity (80%) area of the greenhouse. After two months, the acclimatized plantlets were shifted to earthen pots containing autoclaved sand and garden soil (1 : 1). The plantlets were further maintained in shade house for two months and eventually shifted to the field.

2.6. Foliar Micromorphological Evaluation

In vitro regenerated leaves were used to study the vein density, venation pattern, and types of trichomes at rooting stage after 4 weeks of incubation. The entire leaves were preserved in formalin acetic acid (FAA) solution and cleared in 70% ethanol (v/v) to remove chlorophyll content, bleached with 5% (w/v) NaOH and rinsed in water until the plant material is free from NaOH. The leaves were then stained with 1% safranin (Loba Chemie, India) and mounted in water and examined under the microscope (Labomed iVu 3100, USA).

2.7. Data Collection and Statistical Analysis

Experiments were laid out in completely randomized block design [23] and repeated thrice. Each treatment consisted of minimum ten replicates. The observations on response of explants, number of shoots and their height, percentage of rooted shoots, and root length were recorded after a regular time interval of 4 weeks. Analysis of variance and Duncan’s multiple range tests were used for comparison among resulting mean values.

3. Results and Discussion

3.1. Establishment of Cultures

Surface sterilization of the explants for 4 min and trimming both the cut ends reduced the rate of contamination. Bud breaking from nodal meristems was observed in all the explants with all the concentrations of growth regulators within 7 days of inoculation, whereas no shoots were developed on MS basal medium devoid of growth regulators.

The percentage of bud breaking from nodal explants was increased while increasing the concentration of cytokinins, both BAP (up to 1.0 mg L⁻¹) and Kin (up to 1.5 mg L⁻¹), and decreased with higher concentrations. However, the percentage of culture responses was low on Kin (76%) compared to BAP (98%). Maximum 3.2 shoots with 4.3 cm average length resulted from MS medium augmented with BAP alone at 1.0 mg L⁻¹ (Table 1). Benzylaminopurine was found better than Kin in terms of percentage response as well as number of shoots per explant. The superiority of BAP over Kin for bud break as well as shoot growth and multiplication has also been reported in Cyclea peltata [24] and Morinda citrifolia [25]. The number of shoots induced per explant varied in all the treatments. The length of axillary shoots regenerated from explants varied from 1.5 to 4.3 cm on MS medium with all the concentrations of BAP (Figure 1(a)). Only two shoots with 2.2 cm length were recorded with Kin, and the shoot lengths were varied from 1.7 to 2.8 cm. Increased concentrations of cytokinins inhibited the overall response of explants. This type of adverse effects of higher concentration of cytokinins at initiation stage has been reported in Celastrus paniculatus [26], Caralluma edulis [27], and Passiflora foetida [28].

Table 1: Effect of cytokinins on induction of shoots from nodal segments of R. pectinata.

Conc. of cytokinins (mg L⁻¹)
Response (%)
Shoot number (mean SD)
Shoot length (cm) (mean SD)

BAP
Kin

0.0
0.0
0
0.0 0.00
0.0 0.00

0.5
—
75
1.2 0.11
3.0 0.20

1.0
—
98
3.2 0.10
4.3 0.13

1.5
—
86
1.7 0.21
3.2 0.21

2.0
—
72
1.0 0.24
2.8 0.14

3.0
—
60
1.2 0.17
1.5 0.21

—
0.5
59
1.5 0.20
1.8 0.10

—
1.0
74
2.0 0.15
2.2 0.26

—
1.5
76
1.2 0.24
2.8 0.14

—
2.0
65
1.4 0.40
2.0 0.31

—
3.0
52
1.0 0.16
1.7 0.19

Note. Mean separation was analyzed by ANOVA using SPSS software (ver. 16.0); the values represented in corresponding column followed by same letters are not significantly different according to DMRT at P < 0.05.

(a)

(b)

(c)

(d)

(e)

Figure 1: (a) Induction of shoots from the nodal meristems of the explants. (b) Multiplication of shoots of R. pectinata. (c) In vitro flowering in R. pectinata. (d) Induction of roots from the in vitro regenerated shoots in half strength MS medium with IBA. (e) Stages in hardening of plantlets in the greenhouse.

3.2. Shoot Multiplication

The newly developed young shoots with explants were harvested and subcultured on fresh MS medium supplemented with BAP, Kin, and IAA. The response of explants at initiation stage indicated the significance of BAP in the multiplication medium. But significant increase in number of shoots was observed when the medium was incorporated with Kin and IAA along with BAP. The addition of IAA with BAP and Kin further improved the rate of shoots multiplication. Kataria and Shekhawat [29] reported the efficacy of BAP and IAA in shoot multiplication of Rauvolfia serpentina.

Maximum number of shoots (13.2) was observed on MS medium supplemented with 0.5 mg L⁻¹ each of BAP and Kin and 0.1 mg L⁻¹ IAA in this study (Table 2 and Figure 1(b)). The positive response and number of shoots with maximum length per culture showed a continuous increase in each subculture up to the fourth subculture, and thereafter it decreased. Repeated subcultures resulted in increase in number of multiple shoots. Recently Shekhawat et al. [25] and Patel et al. [27] had successfully used this technique to increase the shoot numbers in M. citrifolia and Caralluma edulis. They observed amplification of shoot numbers up to the third subculture stage. Similar observations were also made in different species such as Pterocarpus santalinus [30], Justicia gendarussa [31], and Eulophia nuda [32].

Table 2: Effect of different concentrations of cytokinins (BAP and Kin) combined with IAA on multiplication of shoots.

Conc. of BAP and Kin (mg L⁻¹)
Conc. of IAA (mg L⁻¹)
Shoot number
(mean SD)
Shoot length (cm)
(mean SD)

0
0
0.0 0.0
0.0 0.0

0.25
—
6.3 1.2
5.3 0.4

0.5
—
9.5 1.9
5.9 0.3

1.0
—
7.3 1.0
4.2 0.6

1.5
—
6.6 1.3
4.7 0.1

2.0
—
5.4 1.0
5.0 0.5

0.5
0.1
13.2 1.6
5.2 0.0

0.5
0.2
9.3 0.9
4.5 0.7

0.5
0.3
8.1 1.0
4.0 0.2

0.5
0.4
5.2 0.7
3.5 0.3

Note. Mean separation was analyzed by ANOVA using SPSS software (ver. 16.0); the values represented in corresponding column followed by same letters are not significantly different according to DMRT at P < 0.05.

3.3. In Vitro Flowering in Cultures

Medium strength, growth regulators, and specific photoperiod had significant impact on in vitro flowering. The shoots (5-6 cm length) isolated from third subculture on half strength MS medium supplemented with 0.5 mg L⁻¹ each of BAP and Kin + 0.1 mg L⁻¹ IAA only responded in flowering. Among the photoperiods studied for flower induction in vitro, 12/12 hr light/dark photoperiod with 30 μmol m⁻² s⁻¹ SFPD light intensity was found best. The in vitro induced flowers were morphologically similar to those of the plants in the field. Similar reports were published in Vitex negundo [33] and Ipomoea sepiaria [18]. The effect of photoperiod on in vitro flowering has also been studied in Psygmorchis pusilla [12]. About 80% shoots were responded in in vitro flowering in the present study (Table 3). The in vitro shoots end with the single inflorescence as in the naturally grown plants (Figure 1(c)).

Table 3: Effect of photoperiod on in vitro flowering of R. pectinata on half strength MS medium after 4 weeks of culture.

Photoperiod (hr/d) (light/dark)
Percentage of shoots producing inflorescence

12/12
80

16/8
68

8/16
00

3.4. In Vitro Rooting of Shoots and Hardening of Plantlets

The healthy shoots measuring 5-6 cm in length were used to induce roots by culturing on auxins supplemented medium. The shoots separated from third subculture responded better in this experiment. Maximum response in root induction was achieved when half strength MS medium was supplemented with 2.0 mg L⁻¹ IBA. About 95% of shoots were rooted with 4.9 roots per shoot (3.5 cm length) on this medium combination (Table 4 and Figure 1(d)). IBA was found better in root induction response and number and length of roots compared to all concentrations of IAA and NAA evaluated for rooting efficiency. Maximum 2.8 roots with 2.14 cm length were induced with 67% response on MS medium incorporated with 1.0 mg L⁻¹ NAA. But 3.6 roots with 2.0 cm length were recorded with 3.0 mg L⁻¹ IAA. The superiority of IBA among other auxins has been reported in M. citrifolia [25] and Ipomoea sepiaria [18].

Table 4: Effect of auxins on in vitro root induction of R. pectinata on half strength MS medium.

PGR and its concentration (mg L⁻¹)
Response (%)
Root number
(mean SD)
Root length (cm) (mean SD)

0
0
0.00 0.00
0.00 0.00

IAA

    1.0
60
2.5 0.16
1.10 0.24

    2.0
72
2.8 0.21
2.80 0.17

    3.0
69
3.6 0.29
2.00 0.22

    4.0
60
2.4 0.10
1.28 0.38

IBA

    1.0
91
3.7 0.13
2.71 0.29

    2.0
95
4.9 0.22
3.50 0.15

    3.0
87
3.2 0.10
3.00 0.40

    4.0
70
2.6 0.07
2.50 0.23

NAA

    1.0
67
2.8 0.21
2.14 0.41

    2.0
75
2.6 0.30
2.37 0.23

    3.0
68
2.7 0.33
2.15 0.45

    4.0
61
2.0 0.24
1.40 0.19

Note. Mean separation was analyzed by ANOVA using SPSS software (ver. 16.0); the values represented in corresponding column followed by same letters are not significantly different according to DMRT at P < 0.05.

After four weeks of incubation in rooting medium, the in vitro rooted plantlets were separated from culture vessels and the remnants of medium were removed cautiously and placed in autoclaved Soilrite. These were initially moistened with one-fourth MS salts solution and maintained in high humidity area of the greenhouse for two months. The acclimatized plantlets were shifted to earthen pots (Figure 1(e)) containing autoclaved sand and garden soil (1 : 1). Finally the hardened plantlets were shifted to the field.

3.5. Foliar Micromorphological Study

The epidermal cells of the leaves were large and thick and possessed characteristic diacytic stomata surrounded by two distinct subsidiary cells at the two poles of the guard cells. Trichomes were observed along with the veins and secondary veins. Two types of uniseriate trichomes, unicellular glandular and multicellular nonglandular trichomes, were observed. The glandular trichomes were spherical in shape and consisted of unicellular head and subsessile stalk. The nonglandular trichomes were long and consisted of thick-walled broader cells with cuneate base and pointed apex. Glandular trichomes were more frequent than the nonglandular trichomes (Figures 2(a) and 2(b)). Amit and Daniel [34] reported the presence of diacytic stomata and glandular and nonglandular trichomes in Rungia repens. The presence of trichomes was considered as indicative on the concentration of secondary metabolites and as important biomarkers in plant identification [35]. Glandular trichomes with empty cells were also reported in Rungia repens by Dipa and Daniel [36].

(a)

(b)

Figure 2: (a) Venation pattern in leaves of in vitro raised shoots; (b) multicellular, nonglandular trichome (scale bar 50.0 µm, 100.0 µm).

The cystoliths present in the petioles of R. pectinata were reported by A. M. Patil and D. A. Patil [37] and Metcalfe and Chalk [38] and their significance was studied by Ahmad [39] but no cystoliths were observed in the present experiment. Large and distinct vein-islets were reported with polygonal areoles (islets). The in vitro environment at rooting stage enhances the area of polygonal regions by meristematic growth and each becomes subdivided into loops. The vein-islets adjacent to margin do not show loop formation (Figure 2(a)). It is understood that the acclimatization processes further enhance the vein-islet density and favor the plantlet growth in the field. The architectural properties of leaf venation are related to functional aspects. The leaf venation pattern of R. pectinata indicates strong selective pressures acting on the architectural arrangement of the conducting bundles of the leaf at rooting stage. Pospíšilová [40] and Wang et al. [41] reported that the application of cytokinins in culture medium significantly affects rate of transpiration.

Wax deposition, transpiration from leaves, stomatal functionality, and changes in structure after transplantation in the ex vitro and field conditions were studied in number of plants [42–44]. So the knowledge of various functional features of leaf venation pattern could enhance the survival rate of the micropropagated plants in the field.

3.6. Conclusion

Tissue culture protocol has been successfully developed for R. pectinata in this study. The regenerated shoots were subjected to induction of in vitro flowering. The plantlets were hardened and field-transferred. The foliar micromorphological study was conducted to understand the developmental changes during in vitro culture at rooting stage.

Abbreviations

BAP: | 6-Benzylaminopurine
Kin: | Kinetin
IAA: | Indole-3-acetic acid
IBA: | Indole-3-butyric acid
NAA: | -Naphthalene acetic acid
MS medium: | Murashige and Skoog [22] medium
SFPD: | Spectral Flux Photon Density
FAA: | Formalin acetic acid.

Disclosure

The present research work has not involved any human participants and/or animals.

Competing Interests

The authors report that there are no competing interests regarding the publication of this paper.

Acknowledgments

The authors are grateful to the Department of Science, Technology and Environment, Government of Puducherry, for providing financial support as Grant-in-Aid Scheme.

References

J. S. Gamble, Flora of the Presidency of Madras, Adlard, London, UK, 1921.

H. O. Saxena and M. Brahman, The Flora of Orissa, Bhubaneswar, India, Orissa Forest Development Corporation, 1995.

J. B. Harborne, Phytochemical Methods: A Guide to Modern Techniques of Plant Analysis, Chapman and Hall, New York, NY, USA, 1984.

S. R. Swain, B. N. Sinha, and P. N. Murthy, “Comparative evaluation of anti-pyretic and analgesic activities of Rungia repens Nees and Rungia pectinata Linn,” Asian Journal of Pharmaceutical and Clinical Research, vol. 4, no. 2, pp. 103–106, 2011.

K. M. Nadkarni, Indian Materia Medica, Popular Prakashan, Mumbai, India, 2002.

The Wealth of India (Raw Materials), CSIR, New Delhi, India, 1999.

G. E. Trease and W. C. Evans, Pharmacognosy, WB Saunders, Philadelphia, Pa, USA, 15th edition, 2002.

S. R. Swain, B. N. Sinha, and P. N. Murthy, “Antiinflammatory, diuretic and antimicrobial activities of Rungia pectinata linn. and Rungia repens Nees,” Indian Journal of Pharmaceutical Sciences, vol. 70, no. 5, pp. 679–683, 2008.

A. Singh, M. K. Singh, and R. Singh, “Traditional medicinal flora of the district Buxar (Bihar, India),” Journal of Pharmacognosy and Phytochemistry, vol. 2, no. 2, pp. 41–49, 2013.

B. S. Adhikari, M. M. Babu, P. L. Saklani, and G. S. Rawat, “Medicinal plants diversity and their conservation status in Wildlife Institute of India (WII) campus, Dehradun,” Ethnobotanical Leaflets, vol. 14, no. 1, pp. 46–83, 2010.

B. Tisserat and P. D. Galletta, “In vitro flowering and fruiting of Capsicum frutescens L,” Horticultural Science, vol. 30, no. 1, pp. 130–132, 1995.

A. P. A. Vaz, R. D. C. L. Figueiredo-Ribeiro, and G. B. Kerbauy, “Photoperiod and temperature effects on in vitro growth and flowering of P. pusilla, an epiphytic orchid,” Plant Physiology and Biochemistry, vol. 42, no. 5, pp. 411–415, 2004.

A. Sharma, V. Kumar, P. Giridhar, and G. A. Ravishankar, “Induction of in vitro flowering in Capsicum frutescens under the influence of silver nitrate and cobalt chloride and pollen transformation,” Electronic Journal of Biotechnology, vol. 11, no. 2, pp. 1–6, 2008.

M. A. Z. Munsur, M. S. Haque, K. M. Nasiruddin, and M. S. Hossain, “In vitro propagation of bitter gourd (Momordica charantia L.) from nodal and root segments,” Plant Tissue Culture and Biotechnology, vol. 19, no. 1, pp. 45–52, 2009.

S. Mondal, J. A. T. Silva, and P. D. Ghosh, “In vitro flowering in Rauvolfia serpentina (L.) Benth. ex. Kurz,” International Journal of Plant Developmental Biology, vol. 5, no. 1, pp. 75–77, 2011.

M. S. Shekhawat, “Induction of in vitro flowering in Arnebia hispidissima (Lehm.) DC,” International Journal of BioScience and Technology, vol. 5, no. 16, pp. 88–92, 2012.

D. Kaur, P. Thapa, M. Sharma, A. Bhattacharya, and A. Sood, “In vitro flowering—a system for tracking floral organ development in Dendrocalamus hamiltonii Nees et Arn. ex Munro,” Indian Journal of Experimental Biology, vol. 52, no. 8, pp. 825–834, 2014.

M. K. Cheruvathur, J. Abraham, and T. D. Thomas, “In vitro micropropagation and flowering in Ipomoea sepiaria Roxb. An important ethanomedicinal plant,” Asian Pacific Journal of Reproduction, vol. 4, no. 1, pp. 49–53, 2015.

M. S. Lamhamedi, H. Chamberland, and F. M. Tremblay, “Epidermal transpiration, ultrastructural characteristics and net photosynthesis of white spruce somatic seedlings in response to in vitro acclimatization,” Physiologia Plantarum, vol. 118, no. 4, pp. 554–561, 2003.

B. N. Hazarika, “Acclimatization of tissue-cultured plants,” Current Science, vol. 85, no. 12, pp. 1704–1712, 2003.

J. Pospíšilová, I. Tichá, P. Kadleček, D. Haisel, and Š. Plzáková, “Acclimatization of micropropagated plants to ex vitro conditions,” Biologia Plantarum, vol. 42, no. 4, pp. 481–497, 1999.

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.

M. E. Compton and C. W. Mize, “Statistical considerations for in vitro research: I—birth of an idea to collecting data,” In Vitro Cellular and Developmental Biology—Plant, vol. 35, no. 2, pp. 115–121, 1999.

J. Abraham, M. K. Cheruvathur, B. Mani, and T. D. Thomas, “A rapid in vitro multiplication system for commercial propagation of pharmaceutically important Cyclea peltata (Lam) Hook < Thoms. Based on enhanced axillary branching,” Industrial Crops and Products, vol. 31, no. 1, pp. 92–98, 2010.

M. S. Shekhawat, N. Kannan, M. Manokari, and C. P. Ravindran, “Enhanced micropropagation protocol of Morinda citrifolia L. through nodal explants,” Journal of Applied Research on Medicinal and Aromatic Plants, vol. 2, no. 4, pp. 174–181, 2015.

M. Phulwaria, M. K. Rai, A. K. Patel, V. Kataria, and N. S. Shekhawat, “A genetically stable rooting protocol for propagating a threatened medicinal plant—Celastrus paniculatus,” AoB Plants, vol. 5, Article ID pls054, 2013.

A. K. Patel, M. Phulwaria, M. K. Rai, A. K. Gupta, S. Shekhawat, and N. S. Shekhawat, “In vitro propagation and ex vitro rooting of Caralluma edulis (Edgew.) Benth. & Hook. f.: an endemic and endangered edible plant species of the Thar Desert,” Scientia Horticulturae, vol. 165, pp. 175–180, 2014.

M. S. Shekhawat, N. Kannan, M. Manokari, and C. Ravindran, “In vitro regeneration of shoots and ex vitro rooting of an important medicinal plant Passiflora foetida L. through nodal segment cultures,” Journal of Genetic Engineering and Biotechnology, vol. 13, no. 2, pp. 209–214, 2015.

V. Kataria and N. S. Shekhawat, “Cloning of Rauvolfia serpentina—an endangered medicinal plant,” Journal of Sustainable Forestry, vol. 20, no. 1, pp. 53–65, 2005.

E. Prakash, P. S. Sha Valli Khan, T. J. V. Sreenivasa Rao, and E. S. Meru, “Micropropagation of red sanders (Pterocarpus santalinus L.) using mature nodal explants,” Journal of Forest Research, vol. 11, no. 5, pp. 329–335, 2006.

T. D. Thomas and H. Yoichiro, “In vitro propagation for the conservation of a rare medicinal plant Justicia gendarussa burm. f. by nodal explants and shoot regeneration from callus,” Acta Physiologiae Plantarum, vol. 32, no. 5, pp. 943–950, 2010.

D. Panwar, K. Ram, Harish, and N. S. Shekhawat, “In vitro propagation of Eulophia nuda Lindl., an endangered orchid,” Scientia Horticulturae, vol. 139, pp. 46–52, 2012.

M. S. Rathore and N. S. Shekhawat, “Micropropagation of Vitex negundo through in vitro bud proliferation,” Agricultural Science Research Journals, vol. 1, no. 8, pp. 191–198, 2011.

G. Amit and M. Daniel, “Identification of pharmacognostic and phytochemical biomarkers,” International Journal of Pharmaceutical, Biological and Chemical Sciences, vol. 3, no. 2, pp. 58–64, 2014.

D. Gohil, V. M. Raole, and M. Daniel, Micromorphological Characters as Biomarkers for Some of the Medicinal Plants of Gujarat, Herbal Technology: Recent Trends and Progress, 2007.

C. Dipa and M. Daniel, “Foliar trichomes of some members of the family Acanthaceae and their taxonomic utility,” International Journal of Pharma and BioSciences, vol. 2, no. 3, pp. 231–235, 2011.

A. M. Patil and D. A. Patil, “Occurrence and significance of cystoliths in Acanthaceae,” Current Botany, vol. 2, no. 4, pp. 1–5, 2011.

C. R. Metcalfe and L. Chalk, Anatomy of Dicotyledons, vol. 1, no. 6, Clarendon Press, Oxford, UK, 1950.

K. J. Ahmad, “Taxonomic significance of epidermal characters in Acanthaceae,” in Progress in Plant Research, vol. 1, pp. 135–160, Today and Tomorrow’s Printers and Publishers, New Delhi, India, 1979.

J. Pospíšilová, “Interaction of cytokinins and abscisic acid during regulation of stomatal opening in bean leaves,” Photosynthetica, vol. 41, no. 1, pp. 49–56, 2003.

G. Wang, C. Li, and F. Zhang, “Effects of different nitrogen forms and combination with foliar spraying with 6-benzylaminopurine on growth, transpiration, and water and potassium uptake and flow in tobacco,” Plant and Soil, vol. 256, no. 1, pp. 169–178, 2003.

M. Ziv, “In vitro hardening and acclimatization of tissue cultured plants,” in Plant Tissue Culture and Its Agricultural Applications, L. A. Withers and P. G. Anderson, Eds., pp. 187–196, Butterworths, London, UK, 1986.

J. Pospíšilová and P. Baťková, “Effects of pre-treatments with abscisic acid and/or benzyladenine on gas exchange of French bean, sugar beet, and maize leaves during water stress and after rehydration,” Biología Plantarum, vol. 48, no. 3, pp. 395–399, 2004.

J. Ďurkovič, A. Lengyelová, I. Čaňová, D. Kurjak, and D. Hladká, “Photosynthetic performance and stomatal characteristics during ex vitro acclimatisation of true service tree (Sorbus domestica L.),” Journal of Horticultural Science and Biotechnology, vol. 84, no. 2, pp. 223–227, 2009.