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 Table of Contents  
ORIGINAL ARTICLE
Year : 2020  |  Volume : 12  |  Issue : 3  |  Page : 324-334  

Micropropagation, myristicin production enhancement, and comparative GC-MS analysis of the n-hexane extracts of different organs of Daucus pumilus (Gouan), family Apiaceae


Department of Pharmacognosy, Faculty of Pharmacy, Zagazig University, Zagazig 44519, Egypt

Date of Submission09-Nov-2019
Date of Decision09-Mar-2020
Date of Acceptance08-Apr-2020
Date of Web Publication20-Jul-2020

Correspondence Address:
Dr. Sahar Abdelaziz
Department of Pharmacognosy, Faculty of Pharmacy, Zagazig University, Zagazig.
Egypt
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Source of Support: None, Conflict of Interest: None


DOI: 10.4103/jpbs.JPBS_289_19

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   Abstract 

Aim: This work aimed to study the somatic embryogenesis and organogenesis of endangered Daucus pumilus (Gouan) for the conservation of this plant and improving the production of secondary metabolites of medicinal value. Materials and Methods: The callus formation and in vitro propagation of D. pumilus (Gouan) by using a different combination of naphthalene acetic acid and benzylaminopurine were established. Various embryogenic stages were tracked using scanning electron microscopy and light microscopy. The volatile constituents of the n-hexane extracts of D. pumilus (Gouan) that extracted by ultrasonic-assisted technique were analyzed by gas chromatography–mass spectrometry. Results and Discussion: Somatic embryogenesis and organogenesis of endangered D. pumilus (Gouan) were established for the first time. Myristicin and elemicin were successfully increased during micropropagation to 70.89% and 2.19%, respectively. Furthermore, the induction of compounds such as 6-methoxymellein, eugenin, methyl behenate, and 1,6-dimethylnaphthalene was also detected. Conclusion: Commercially, this protocol decreases the dependence on wild medicinal plants, enhances the manufacturing of valuable phytochemicals to meet the great demands of the pharmaceutical industries, and acts as a mean for genetic transformation of this plant.

Keywords: Daucus pumilus, gas chromatography–mass spectrometry, myristicin, organogenesis, somatic embryogenesis


How to cite this article:
Arafa AM, Abdel-Ghani AE, El-Dahmy SI, Abdelaziz S. Micropropagation, myristicin production enhancement, and comparative GC-MS analysis of the n-hexane extracts of different organs of Daucus pumilus (Gouan), family Apiaceae. J Pharm Bioall Sci 2020;12:324-34

How to cite this URL:
Arafa AM, Abdel-Ghani AE, El-Dahmy SI, Abdelaziz S. Micropropagation, myristicin production enhancement, and comparative GC-MS analysis of the n-hexane extracts of different organs of Daucus pumilus (Gouan), family Apiaceae. J Pharm Bioall Sci [serial online] 2020 [cited 2020 Oct 22];12:324-34. Available from: https://www.jpbsonline.org/text.asp?2020/12/3/324/290124




   Introduction Top


Myristicin is the main constituent of Daucus pumilus (Gouan) volatile oil,[1] which shows various biological activities, such as hepatoprotective, antibacterial, insecticidal, cytotoxic, anti-inflammatory, and anticholinergic.[2] It was reported that D. pumilus (Gouan) is endangered in the Maltese Islands,[3] Provence-Alpes-Côte d’Azur[4] and Jordan.[5] Also, D. pumilus (Gouan) is threatened in Egypt[6] and became scarce in Lebanon.[7] In Egypt, the biota of ecosystems has been destroyed in large areas along the coastal regions. This sounds the alarm for the conservation of medicinal plants in the Egyptian coastal dunes.[8] Plant tissue culture techniques enable the repositioning of endangered species and provide a tool for improving the production of metabolites. In addition, these techniques can produce novel compounds that are not naturally synthesized in plants through manipulation of in vitro culture conditions.[9] On the basis of the previous literature, the micropropagation of D. pumilus (Gouan) has not been studied. Hence, the first aim of this work was to study the in vitro seed germination, callus induction, and regeneration of D. pumilus. Moreover, investigation of phytochemical production in D. pumilus (Gouan) by chemical analysis was the second important goal of this study.


   Materials and Methods Top


Plant material

The plant material of wild D. pumilus (Gouan) (Pseudorlaya pumila (L.) Grande)[10] (family: Apiaceae) was collected in March 2014 from the west of Edku, the Beheira Governorate, Egypt. Fruits enclosing seeds were cultivated in the medicinal farm of the Pharmacognosy Department, Faculty of Pharmacy, Zagazig University, Egypt. The plant was identified by Dr. Hasnaa Hosni, Professor of Plant Taxonomy, Botany Department, Faculty of Science, Cairo University, Egypt. A voucher specimen (Accession number of PU-101) was deposited in the Herbarium of the Department of Pharmacognosy, Faculty of Pharmacy, Zagazig University, Egypt.

Sterilization of seeds

Wild fruits enclosing seeds of D. pumilus (Gouan) were separated into individual mericarps and then sterilized by immersion in 70% ethyl alcohol for 3 min, followed by shaking with 5% sodium hypochlorite solution (Clorox, Okland, CA, USA) containing two drops of 1% tween 20 for 20 min. Under a laminar flow cabinet, the hypochlorite solution was removed, and then the seeds were rinsed three times with sterile distilled water before germination.

Seed germination in vitro

Each sterilized mericarp enclosing seeds was cut transversely into two parts and then cultured on sterile Murashige and Skoog (MS) medium (Duchefa Biochemie B.V., Harlem, the Netherlands),[11] supplemented with 30g/L sucrose (Adwic, Cairo, Egypt) and 8g/L agar (purified agar for plant tissue culture, BioWorld, Visalia, CA, USA), either alone or in combination with 50 mg/L of gibberellic acid (GA3). The pH was adjusted to 5.8 by 1N HCl or 1N NaOH solution using a Jenway 3510 pH meter before autoclaving at 121°C for 20 min. Four replicates of 26 mericarps enclosing seeds were used for each experiment. All jars were incubated at 25±2°C under a 16 h photoperiod using a white fluorescent lamp. Radicle protrusion of approximately 2mm was used as a guide for germination of seeds. Seed germination percentage was assessed using the equation reported by Pattanaik et al.[12]

Induction and maintenance of callus

Five-week-old seedlings were aseptically dissected into small parts (0.5–1cm) and used as explants for callus formation. Explants were cultivated on sterile MS media containing 3% sucrose, 0.8% agar, and supplemented with various growth regulators (Sigma Chemical, St. Louis, Missouri, USA) combinations as medium I: 0.4 mg/L naphthalene acetic acid (NAA) + 4 mg/L 6-benzylaminopurine (BAP); medium II: 0.1 mg/L NAA+ 1 mg/L BAP; medium III: 1 mg/L NAA+ 0.1 mg/L BAP; medium IV: 2 mg/L 2 mg/L 2, 4 dichlorophenoxy acetic acid (2,4 D) + 1 mg/L kinetin (Kin) and medium V: 0.5 mg/L thidiazuron (TDZ) + 1 mg/L 2, 4 D + 0.1 mg/L BAP. All media were adjusted to a pH of 5.8, and the cultures were maintained at 25±2°C under 16 h of daily light. Four explants in each jar with four replicates were used for each treatment. Callus cultures were transferred to fresh medium with the same composition every 4 weeks to induce proliferation. The callus induction percentage was measured according to the formula stated by Atabaki et al.[13]

Growth parameters determination

The growth curve, growth index (GI), specific growth rate, and doubling time (dt) are kinetic tools for evaluating callus growth. Subculturing of induced calli was performed for 2 to 3 generations as a multiplication step before scoring the data. The growth curve was established by plotting the mean value of three replicates of either fresh or dry weight against time. The GI, specific growth rate (μ), and dt were calculated according to equations reported by Godoy-Hernández and Vázquez-Flota.[14]

In vitro propagation of Daucus pumilus (Gouan)

Indirect somatic embryogenesis

After 12–14 weeks on media I, II and III, green embryogenic calli with nodular structures were selected and subcultured on media of the same composition every 28 days for 10 weeks, where development of somatic embryos was monitored by light microscopy. For germination, somatic embryos were transferred to sterile hormone-free MS (HF) medium containing 30g/L sucrose and 6g/L agar with a pH of 5.8. Subculturing on fresh media of the same composition was performed twice for 8 weeks.

Indirect organogenesis

The non-embryogenic calli on media I and II were carefully subcultured on the same media for 12–16 weeks until the formation of shoot buds. These buds were transferred to medium III or sterile MS solid medium supplemented with 1 mg/L NAA for 8–10 weeks and subcultured every 3 weeks on the same fresh media. All cultures for somatic embryogenesis or organogenesis were maintained at 25±2°C under a white fluorescent lamp with a 16 h photoperiod.

Scanning electron microscopy

Embryogenic calli were prepared for scanning electron microscopy (SEM) according to the general methods for biological sample preparation.[15]

Hardening and acclimatization of the in vitro regenerated plantlets

Two-month-old rooted plantlets were washed with sterile distilled water and out-planted in perforated pots containing autoclaved peat moss soil and sand (1:1). Pots were covered with transparent polyethylene plastic bags to maintain humidity. They were maintained in a growth chamber (25°C and 16 h photoperiod) and irrigated every 2 days with sterile distilled water. After 2 weeks, transparent plastic bags were removed gradually. Finally, pots were transferred to the greenhouse and regularly irrigated to maintain sufficient soil moisture.

Ultrasonic-assisted extraction of volatile constituents

Wild and cultivated D. pumilus (Gouan) fruit, collected leaves and stems, 12-week-old non-organogenic calli (cultivated on media I, II and III), and 8-week-old in vitro regenerated plantlets were extracted separately (each of 25g) with n-hexane (3 × 150 mL) in a 250-mL volumetric flask and placed in an ultrasonic bath (Sonorex Super RK 103 H, Bandelin, Germany) with a frequency of 35 KHz and a power of 140 W for 15 min at a temperature of 40°C. After ultrasonic-assisted extraction, flasks were kept on a shaker overnight, and the contents were filtered and concentrated by a rotary evaporator (Heidolph rotavapor, Schwabach, Germany) at 45°C and 100rpm. Hexane extracts were stored in a refrigerator at –4°C until analysis.

Gas chromatography–mass spectrometry analysis

An Agilent 6890 gas chromatograph equipped with an Agilent mass spectrometric detector with a direct capillary interface and fused silica capillary column PAS-5ms (30 m×0.32mm ×0.25 µm film thickness) was used for analysis. Samples were dissolved in n-hexane (100 µL/mL), and 1 µL was injected for each sample. Helium was used as the carrier gas at approximately 1 mL/min in pulsed splitless mode, and the solvent delay was 3 min. The mass spectrometric detector was operated in electron impact ionization mode with an ionizing energy of 70 e.v. scanning from 50 to 500 m/z. The ion source temperature was 230°C. The electron multiplier voltage (EM voltage) was maintained at 1250 V above autotune. The instrument was manually tuned using perfluorotributylamine (PFTBA). The GC temperature program started at 45°C (isothermal for 3 min) and increased to 280°C at 8°C/min, and finally was held isothermally for 10 min. The detector and injector temperatures were set at 280 and 250°C, respectively. The identification of the separated peaks was carried out by matching their mass spectra with those in the literature[16] and mass spectral databases of Wiley and Nist 05. A homologous series of n-alkanes (C8–C24) were injected under similar GC/MS conditions to calculate the retention indices (RI) and were compared with those available in the reported data[16] for further confirmation. The area under the peaks was used to calculate the approximate quantities of the samples using the normalization method.


   Results and Discussion Top


In vitro seed germination and callus induction

After 5 weeks and 2 days, sterilized dissected seeds were germinated on sterile solid MS medium supplemented with 50 mg/L GA3 only (germination percentage of 12%), as shown in [Figure 1]A. The low germination percentage in the Apiaceae is due to the presence of seeds lacking embryos (nonviable) or with rudimentary embryos (immature) or dormant embryos.[17] Exogenous application of gibberellic acid (GA3) can break the seed dormancy by allowing oxygen penetration from the outside to the embryo. Furthermore, GA3 has a role in counteracting the inhibitory effect of abscisic acid (ABA). ABA has a main role in the induction of seed dormancy and its maintenance.[18] GA3 can overcome the dormancy of many Apiaceae seeds.[19][Figure 1]B shows the seedlings with developed cotyledonary leaves and roots, which reached 3–4cm in length within 2 weeks and 5 days from germination. After another 2 weeks, the seedlings with true leaves reached 6–7cm [Figure 1]C. Induction of calli [Figure 1]D–F] was only observed when explants excised from 5-week-old seedlings were cultured on media I, II, and III. Pale green friable calli were induced on medium III within 6 weeks. Media I and II produced yellowish-green compact calli after 8 weeks. Media I and III showed the highest callus induction percentage (100%). However, medium II showed only 75% callus induction.
Figure 1: Stages of in vitro germination of Daucus pumilus (Gouan) seeds and callus induction of their seedling explants. (A) Radicle formation after 5 weeks and 2 days. (B) Seedling of 2 weeks and 5 days. (C) Seedling of 5 weeks old. (D, E) Callus induction on media I and II after 8 weeks, respectively. (F) Callus induction on medium III after 6 weeks

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Growth parameter determination

Medium III was the best one for growth, as it showed 6.2- and 11.11-fold increases in callus production in terms of fresh and dry biomass, respectively, during cultivation for 40 days [Figure 2]A-C. [Table 1] shows other growth parameters, such as GI, specific growth rate (μ), and dt for all media. Lower dt and higher GI and specific growth rate were observed in calli inoculated on medium III. These previous results confirmed that medium III produced fast-growing calli.
Figure 2: Growth curves of Daucus pumilus (Gouan) calli cultivated on medium I (A), medium II (B), and medium III (C). Each data point shows the mean ± standard deviation of three replicates

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Table 1: Growth parameters of Daucus pumilus (Gouan) calli cultivated on media I, II, and III

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In vitro propagation of Daucus pumilus (Gouan)

Indirect somatic embryogenesis

Indirect somatic embryogenesis of D. pumilus (Gouan) [Figure 3] included formation of pro-embryogenic callus with a globular stage at the induction step within 12 weeks on media I and II and 14 weeks on medium III after a period of callus induction on these media. Notably, a combination of NAA and BAP was efficient at inducing and maintaining somatic embryogenesis. This previous result agrees with those of Shekhawat and Manokari.[20] Embryo development and maturation involved the morphological transitions from globular to heart-shaped to torpedo-shaped, and ultimately cotyledonary stages after another 8 weeks on all media [Figure 3]A–D. Stages of somatic embryogenesis [Figure 3]E–I were monitored by light microscopy. Within another 2 weeks, all the media showed formation of germinated embryos with elongated radicles [Figure 3]J and K. For the formation of plantlets with well-developed shoots and roots [Figure 3]L, germinated embryos were transferred into HF medium for 3 weeks. After another 2 weeks, differentiated plantlets with rootlets [Figure 3]M and N were formed on the same medium. Moreover, umbels of white flowers [Figure 3]O were also formed on the lateral shoots after another 1 week on HF medium. Then, two weeks later, fruits were formed [Figure 3]P and Q on the same medium. Similarly, in vitro flower induction on HF medium has been described in many studies[21] and may be related to the endogenous level of auxin.[22] In addition, in vitro flowering of Pimpinella tirupatiensis,[23]Dendrocalamus hamiltonii, and Brassica nigra[20] via somatic embryogenesis was achieved. Furthermore, the regeneration of several plants belonging to the Apiaceae was established through somatic embryogenesis.[24]
Figure 3: Somatic embryogenesis and plant regeneration in Daucus pumilus. Embryogenic calli cultivated on medium I (A), medium II (B), and medium III (C). (D) Cotyledonary-shaped embryo, stages of somatic embryos by light microscope including globular (E), heart-shaped (F), torpedo-shaped (G), and cotyledonary (H,I). (J, K) Germinated embryo with elongated radicle. (L) Differentiated plantlets after 3 weeks on hormone-free (HF) medium. (M, N) Differentiated plantlets with rootlet formation after 5 weeks on HF medium. (O) Umbels of white flower formation after 6 weeks on HF medium. (P, Q) Fruit formation after 8 weeks on HF medium

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Indirect organogenesis

Organogenic calli of D. pumilus (Gouan) were formed with shoot buds on media I and II after 12 and 16 weeks, respectively [Figure 4]A and B, respectively]. The proliferation of shoots [Figure 4]C was achieved after the transfer of shoot buds to medium III and medium supplemented with 1 mg/L NAA within 2 and 3 weeks, respectively. The synergistic effect of cytokinin (BAP) in combination with auxin (NAA) in medium III led to an increase in lateral shoot number and elongation compared to that achieved with medium supplemented with NAA only. This finding is in agreement with that reported by Palengara.[25] Moreover, rooting was established on either medium supplemented with 1 mg/L NAA [Figure 4]D or medium III [Figure 4]E within 4 weeks after transfer. The use of 1 mg/L NAA for root formation is consistent with methods reported for D. carota L.[26] While rooting of D. carota subsp. halophilus shoots was established on medium without plant growth regulators.[24] Moreover, medium supplemented with 1 mg/L NAA resulted in the formation of a flower cluster [Figure 4]F of 2–3 flowers within 5 weeks. After 8 weeks on medium III, a cluster of flowers (inflorescence) [Figure 4]G on the main stem and other clusters of 2–3 flowers on the lateral stems were observed. Similarly, in vitro flowering during organogenesis occurred in some plants belonging to Apiaceae.[24] Furthermore, fruit formation was observed after 8 and 10 weeks on medium supplemented with 1 mg/L NAA [Figure 4]H and medium III [Figure 4]I, respectively. In addition, in vitro fruiting of Ammi majus L.[27] via direct organogenesis was the only previous example in Apiaceae. However, many plants belonging to Apiaceae have been regenerated through organogenesis.[24]
Figure 4: Organogenesis and plant regeneration in Daucus pumilus. Calli with shoot buds cultivated on medium I (A) and medium II (B). (C) Shoot formation after transfer to medium III within 2 weeks. (D) Root formation after transfer to medium supplemented with 1 mg/L naphthalene acetic acid (NAA) within 4 weeks. (E) Root formation after transfer to medium III within 4 weeks. (F) Flower formation after 5 weeks on medium with 1 mg/L NAA. (G) Inflorescence on the main broad stem after 8 weeks on medium III. (H) Fruit formation after 8 weeks on medium with 1 mg/L NAA. (I) Fruit formation after 10 weeks on medium III

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Scanning electron microscopy

SEM showed the presence of numerous globular and heart-shaped forms [Figure 5]A and B, respectively]. On the contrary, late heart-shaped [Figure 5]C and D, torpedo-shaped, and cotyledonary forms [[Figure 5]E and F, respectively] were rarely found. Furthermore, this study revealed the efficiency of the combination of NAA and BAP for the induction, development, and maturation of embryogenic calli.
Figure 5: Scanning electron microscopy (SEM) of different stages of somatic embryos in Daucus pumilus (Gouan), including globular (A), heart-shaped (B), late heart-shaped (C, D), torpedo (E), and cotyledonary (F)

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Hardening and acclimatization of the in vitro regenerated plantlets

Only 4% of the plants [Figure 6]A-D survived for 6 weeks after transfer to the greenhouse. Moreover, two-month-old rooted plantlets with fruits [Figure 6]E and F survived for only 2 weeks after transplantation. Similarly, a low survival rate of plants belonging to Apiaceae was reported previously.[28] Moreover, the difficulty in the acclimatization of Apiaceae plants has been attributed to fungal rots.[29]
Figure 6: Hardening and acclimatization of the in vitro regenerated Daucus pumilus (Gouan) plantlets. (A, B) Two-month-old rooted plantlets, (C) plantlets after 2 weeks of transplantation, plantlets started to wilt after 6 weeks (D) or after 10 days (E) of transplantation, (F) 2.5-month-old rooted plantlets with fruits

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Gas chromatography–mass spectrometry analysis

The gas chromatography–mass spectrometry analysis (GC-MS) analysis of the volatile constituents of the n-hexane extracts of the in vitro regenerated plantlets and different organs of wild and cultivated D. pumilus (Gouan) is shown in [Supplementary Table 1 [Additional file 1]]. A total of 39, 44 and 16 compounds were identified for different organs of wild and cultivated D. pumilus (Gouan) and in vitro regenerated plantlets, respectively. The results showed the presence of 23 similar compounds in both wild and cultivated D. pumilus (Gouan). Myristicin was the major constituent of fruits and collected leaves and stems of wild and cultivated D. pumilus (Gouan) at different concentrations (46.12%, 27.66%, 26.98%, and 2.51%, respectively). This difference between wild and cultivated plants may be due to geographic and climatic factors.[30] A noteworthy feature of this study is that the phenylpropanoids; myristicin and elemicin were successfully increased during the micropropagation method to 70.89% and 2.19% in the in vitro regenerated plantlets, respectively. Similar results were reported for Ocimum basilicum plantlets in which the combination of auxin and BAP led to the synthesis of phenylpropanoids (estragole).[31] The induction of compounds such as 6-methoxymellein (0.42%), eugenin (1.31%), methyl behenate (0.48%), and 1,6-dimethylnaphthalene (0.14%) in the in vitro regenerated plantlets of D. pumilus (Gouan) was detected. Furthermore, this study revealed the absence of any volatile constituents in the n-hexane extracts of all calli except for the production of 6-methoxymellein in a percentage of 11.35% and 17.45% in calli growing on media I and II, respectively. Moreover, 7.78% eugenin was produced only in calli cultivated on medium II. Similarly, 6-methoxymellein and eugenin were produced in cultured D. carota L. and in roots of field-grown plants of the same species in response to stresses such as ethylene, methyl jasmonate, 2,4-D, UV-B irradiation and fungal inoculation.[32],[33] Furthermore, new volatile constituents were produced in plantlets of Eucalyptus camaldulensis Dehn. that regenerated from a nodal explant using a combination of NAA and BAP.[34] In addition, carvone was absent in Mentha spicata L. callus, whereas it was produced in the cultured plantlets.[35] In addition, many researchers stated that the biosynthesis of secondary metabolites is dependent on cell differentiation and restricted to specific organs,[36] which explains why myristicin and other volatile constituents in this study were produced in the in vitro regenerated plantlets but not produced in callus.{Table 2}

Regeneration of D. pumilus (Gouan) in vitro was successfully established via indirect somatic embryogenesis and organogenesis for the first time. In vitro flowering and fruiting of D. pumilus (Gouan) are an amazing mean for completing the life cycle of this plant. Consequently, the biosynthetic machinery necessary to produce metabolites can be achieved inside jars without the need for ex vitro acclimatization. GC-MS revealed that myristicin and elemicin were successfully elevated and new compounds were induced in the n-hexane extract of the in vitro regenerated plantlets. Therefore, this result highlights that in vitro cell cultures of D. pumilus (Gouan) can act as biofactories for secondary metabolite production, independent of the availability of wild plants or appropriate climatic conditions. Commercially, this protocol can be used as a tool for the conservation strategy of D. pumilus (Gouan) and to enhance the manufacturing of valuable phytochemicals to meet the great demands of the pharmaceutical industries. In addition, these methods decrease the dependence on wild medicinal plants and acting as a mean for genetic transformation of this plant.

Acknowledgement

We are sincerely grateful to Dr. Hasnaa Hosni, Professor of Plant Taxonomy, Botany Department, Faculty of Science, Cairo University, Egypt for the identification of the plant.

Financial support and sponsorship

Nil.

Conflicts of interest

There are no conflicts of interest.



 
   References Top

1.
Halim A, Moshaly M, Elrady H, Saad A Composition of the essential oil of the fruits of Pseudorlaya pumila (L.) Grande growing in Egypt. Egypt J Pharma Sci 1991;32:745-50.  Back to cited text no. 1
    
2.
Lee JY, Park W Anti-inflammatory effect of myristicin on RAW 264.7 macrophages stimulated with polyinosinic-polycytidylic acid. Molecules 2011;16:7132-42.  Back to cited text no. 2
    
3.
Schembri PJ, Sultana J Red data book for the Maltese Islands. Valletta, Malta: Department of Information; 1989.  Back to cited text no. 3
    
4.
Noble V, Van Es J, Michaud H, Garraud L Liste Rouge de la flore vasculaire de Provence-Alpes-Côte d’Azur. Aix-en-Provence, France: DREAL Provence–Alpes–Côte d’Azur; 2015.  Back to cited text no. 4
    
5.
Taifour H Jordan plant red list. Irbid, Jordan: Royal Botanic Garden; 2017. p. 936.  Back to cited text no. 5
    
6.
Shaltout KH Monitoring the flora of the Omayed Biosphere Reserve and Measures for Rehabilitation: In the proceedings of the International Workshop on Combating Desertification. In: Lee C, Schaaf T, editors. Rehabilitation of degraded drylands and biosphere reserves. Aleppo, Syria: United Nations Educational, Scientific and Cultural Organization (UNESCO); 2002. p. 1-95.  Back to cited text no. 6
    
7.
Ministry of Environment MUU. Biodiversity assessment and monitoring in the protected areas/Lebanon Leb/95/G31. Horsh Ehden Nature Reserve, Lebanese University, Faculty of Science, Lebanese University Press, Beirut, Lebanon; 2004.  Back to cited text no. 7
    
8.
Ahmed DA, Shaltout KH, Kamal SA Mediterranean sand dunes in Egypt: threatened habitat and endangered flora. Life Sci J 2014;11:946-56.  Back to cited text no. 8
    
9.
Isah T, Umar S, Mujib A, Sharma MP, Rajasekharan P, Zafar N, et al. Secondary metabolism of pharmaceuticals in the plant in vitro cultures: strategies, approaches, and limitations to achieving higher yield. Plant Cell Tissue Organ Cult 2018;132:239-65.  Back to cited text no. 9
    
10.
Jafri S, El-Gadi A Flora of Libya. Tripoli, Libya: Al Faatheh University, Faculty of Science Publication; 1985.  Back to cited text no. 10
    
11.
Murashige T, Skoog F A revised medium for rapid growth and bio assays with tobacco tissue cultures. Physiol Plant 1962;15:473-97.  Back to cited text no. 11
    
12.
Pattanaik S, Dash A, Mishra R, Nayak P, Mohanty R Seed germination and seedling survival percentage of Shorea robusta Gaertn. f. in buffer areas of Similipal biosphere reserve, Odisha, India. J Ecosyst Ecography 2015;5:1.  Back to cited text no. 12
    
13.
Atabaki N, Nulit R, Kalhori N, Lasumin N, Sahebi MaA, Rambod . In vitro selection and development of Malaysian salt-tolerant rice (Oryza sativa L. cv. MR263) under salinity. ASAG 2018;2:08-17.  Back to cited text no. 13
    
14.
Godoy-Hernández G, Vázquez-Flota FA Growth measurements: estimation of cell division and cell expansion. In: Loyola-Vargas VM, Ochoa-Alejo N, editors. Plant Cell Culture Protocols. Methods in Molecular Biology. Totowa, NJ: Humana Press; 2012. p. 41-8.  Back to cited text no. 14
    
15.
Murtey MD, Ramasamy P Sample preparations for scanning electron microscopy–life sciences. In: Janecek M, Kral R, editors. Modern electron microscopy in physical and life sciences. London: InTech; 2016.  Back to cited text no. 15
    
16.
Adams RP Identification of essential oil components by gas chromatography/mass spectrometry. 4th ed. Carol Stream, IL: Allured Publishing Corporation; 2007.  Back to cited text no. 16
    
17.
Robinson RW Seed germination problems in the Umbelliferae. Bot Rev 1954;20:531-50.  Back to cited text no. 17
    
18.
Finch-Savage WE, Leubner-Metzger G Seed dormancy and the control of germination. New Phytol 2006;171:501-23.  Back to cited text no. 18
    
19.
Ayuso M, Ramil-Rego P, Landin M, Gallego PP, Barreal ME Computer-assisted recovery of threatened plants: keys for breaking seed dormancy of Eryngium viviparum. Front Plant Sci 2017;8:2092.  Back to cited text no. 19
    
20.
Shekhawat MS, Manokari M Somatic embryogenesis and in vitro flowering in Hybanthus enneaspermus (L.) F. Muell.: a rare multipotent herb. Asian Pac J Reprod 2016;5:256-62.  Back to cited text no. 20
    
21.
Murthy KSR, Kondamudi R, Chalapathi Rao P, Pullaiah T In vitro flowering: a review. J Agric Technol 2012;8:1517-36.  Back to cited text no. 21
    
22.
Awal A, Ali Ahmed AB, Taha RM, Yaacob JS, Mohajer S Effect of adenine, sucrose and plant growth regulators on the indirect organogenesis and on in vitro flowering in “Begonia x hiemalis” fotsch. AJCS 2013;7:691.  Back to cited text no. 22
    
23.
Prakash E, Khan SV, Meru E, Rao K Somatic embryogenesis in Pimpinella tirupatiensis Bal. and Subr., an endangered medicinal plant of Tirumala hills. Curr Sci2001;81:1239-42.  Back to cited text no. 23
    
24.
Tavares AC, Salgueiro LR, Canhoto JM In vitro propagation of the wild carrot Daucus carota L. subsp. halophilus (Brot.) A. Pujadas for conservation purposes. In Vitro Cell Dev Biol Plant 2010;46:47-56.  Back to cited text no. 24
    
25.
Palengara D Foliar regeneration in Centella asiatica (L.) Urban (Apiaceae): an important threatened medicinal herb. Int J Adv Res 2017;5:970-4.  Back to cited text no. 25
    
26.
Pant B, Manandhar S In vitro propagation of carrot (Daucus carota) L. Sci World 2007;5:51-3.  Back to cited text no. 26
    
27.
Pande D, Purohit M, Srivastava P Variation in xanthotoxin content in Ammi majus L. cultures during in vitro flowering and fruiting. Plant Sci 2002;162:583-7.  Back to cited text no. 27
    
28.
Makunga NP, Jäger AK, Van Staden J Micropropagation of Thapsia garganica: a medicinal plant. Plant Cell Rep 2003;21:967-73.  Back to cited text no. 28
    
29.
Irvani N, Solouki M, Omidi M, Zare A, Shahnazi S Callus induction and plant regeneration in Dorem ammoniacum D., an endangered medicinal plant. Plant Cell Tissue Organ Cult 2010;100:293-9.  Back to cited text no. 29
    
30.
Salehi-Arjmand H, Mazaheri D, Hadian J, Majnoon Hosseini N, Ghorbanpour M Essential oils composition, antioxidant activities and phenolics content of wild and cultivated Satureja bachtiarica Bunge plants of Yazd origin. J Med Plants 2014;3:6-14.  Back to cited text no. 30
    
31.
Monfort LEF, Bertolucci SKV, Lima AF, de Carvalho AA, Mohammed A, Blank AF, et al. Effects of plant growth regulators, different culture media and strength MS on production of volatile fraction composition in shoot cultures of Ocimum basilicum. Ind Crops Prod 2018;116:231-9.  Back to cited text no. 31
    
32.
Coxon DT, Curtis RF, Price KR, Levett G Abnormal metabolites produced by Daucus carota roots stored under conditions of stress. Phytochemistry 1973;12:1881-5.  Back to cited text no. 32
    
33.
Fan X, Mattheis JP, Roberts RG Biosynthesis of phytoalexin in carrot root requires ethylene action. Physiol Plant 2000;110:450-4.  Back to cited text no. 33
    
34.
Mubarak EE, Taha RM Eucalyptus camaldulensis Dehn. (Red Gum): micropropagation, and volatile constituents. J Essent Oil Bear Pl 2015;18:713-7.  Back to cited text no. 34
    
35.
Tisserat B, Vaughn SF Growth, morphogenesis, and essential oil production in Mentha spicata L. plantlets in vitro. In Vitro Cell Dev Biol Plant 2008;44:40-50.  Back to cited text no. 35
    
36.
Grzegorczyk-Karolak I, Kuźma Ł, Wysokińska H In vitro cultures of Scutellaria alpina as a source of pharmacologically active metabolites. Acta Physiol Plant 2016;38:7.  Back to cited text no. 36
    


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