Research Article | Open Access
Ashraf S.A. El-Sayed1 , Manal T. El Sayed1, Hend S. Nada2, Abdallah E. Hassan3 and Eman K. Yousef3
1Microbiology Department, Faculty of Science, Zagazig University, 44519, Egypt.
2Microbiology and Immunology Department, Faculty of Veterinary Medicine, Zagazig University, 44519, Egypt.
3Chemistry Department, Faculty of Science, Zagazig University, 44519, Egypt.
J. Pure Appl. Microbiol., 2019, 13 (4): 2055-2063 | Article Number: 5855 | © The Author(s). 2019
Received: 18/09/2019 | Accepted: 19/10/2019 | Published: 16/12/2019

Taxol, a diterpenoid was initially isolated from the bark of Taxus brevifolia, approved by FDA in 1994 as a powerful drug for metastatic ovarian carcinoma, breast and lung cancer. However, due to limitations in the production of this drug based on this plant source, the productive potentiality of fungi of this compound opened a new avenue for its commercial production. In this study, among the twenty fungal isolates screened for Taxol production, Aspergillus terreus had the highest potentiality to produce Taxol (131.2 µg/ml). The productivity of Taxol by A. terreus has been maximized by nutritional optimization using inhibitors and growth regulators. The yield of Taxol by A. terreus was maximally obtained (0.663µg/ml) by growing the fungal isolate on potato dextrose broth medium, amended with addition of biotin at 150 µg/ml for 20 days. The chemical structure Taxol extracted of A. terreus has been verified by proton and carbon NMR, IR and UV analyses. The activity of A. terreus Taxol has been assessed towards multiple cell lines, displaying a strong anticancer activity. In conclusion, the productivity of Taxol by A. terreus has been greatly improved upon using biotin as chemical modulator, that open a new avenue for commercializing the Taxol yield by fungi.


Aspergillus terreus; Taxol; Nutritional optimization, Inhibitors.


Taxol was firstly isolated and chemically identified by X-rays crystallography from the bark of Pacific Yew trees (Taxus brevifolia) (Wani et al., 1971) and approved as a blockbuster anticancer drug for different cancerous types (Brown, 2003). The anticancer activity of Taxol arises from its specificity for binding with tubulin b-subunits, inducing tubulin polymerization, disrupting mitotic division of cancer cells (Straubinger et al., 1993). Although Taxol is produced from the bark of T. brevifolia, its tiny yield and vulnerability to unpredicted fluctuation with the ecological conditions were the major challenges to this approach (Malik et al., 2011; Wang et al., 2011). However, semisynthetic process of 10-deacetylbaccatin III (DAB) intermediates isolated from the European Yew (Taxus baccata) is the current approach for production of Taxol, but the heterogeneity of DAB yield with ecological conditions of T. baccata, the need for wide cultivation area and breading time are the major limitation (Thomas and Polwart, 2003). Alternatively, endophytic fungi from Taxus spp with powerful potency for Taxol production, unlocked a new rout to scale-up the Taxol yield, for their fast growth, cost effectiveness, independency on climat changes, possibility for growing on bulk fermenters, and feasibility for genetic manipulation (Stierle et al., 1993). With the higher applications of Taxol and its derivatives, the global demand of Taxol increases annually by approximately 10%, thus, Taxol sources are the current challenge to sustain its global affordability (El-Sayed et al., 2017). Exploring of the fungal endophytes from Taxol producing and non-producing plants for ability to produce Taxol independent on their plant source and feasibility of metabolic manipulation raised the hope for industrial production of Taxol based on this technology. More than 250 endophytic fungal isolates were identified from T. baccata and about 20% of this population has the potentiality for Taxol production (Caruso et al., 2000; Flores-Bustamante et al., 2010). The biodiversity of fungal endophytes and their Taxol yield have been extensively reported (Strobel et al., 1996; El-Sayed et al., 2018a; Zein et al., 2019; El-Sayed et al., 2019; Artz et al., 2011). Frequent reports claimed the medicinal plants of ethnopharmacological relevance could provide a fertile source for different therapeutics (El-Sayed et al., 2019; El-Sayed et al., 2018). So, exploring novel endophytic fungi from medicinal plants with promising, sustainable potency for Taxol production is the eventual objective. Among the plants of medicinal relevance, Podocarpus spp with ethnopharmacological significance were traditionally used for their activity against bacterial and fungal pathogens, and for cancer treatment (Abdillahi et al., 2010; El-Sayed et al., 2019) . Thus, the objective of this study was to screen the potentiality of endophytic fungi recovered from different medicinal plants, to produce Taxol. As well as to optimize the Taxol yield by the potent fungal isolate using different chemical inhibitors.

Materials and Methods

Isolation and culturing of the endophytic fungi
Different plant types were collected from Sharkia province, Egypt, during June-August/ 2018, as a source of endophytic fungal isolates. These plants were Zea mays, Solanum nigrum, Portulaco oleracea, Convalvulus arrensis, Ocimum basilicum, Erchharnia crassipes, Rosa sp, Citrus xaurantium, and Ricinus communis. The collected plant parts were cut into small segments (5mm) with sterile sharp blade then washed by sterile distilled water and then sterilized with 70% ethanol (v/v) for 2 min, then washed by 2.5% sodium hypochlorite (NaOCl) and dried on sterile filter paper (Xiong et al., 2013). The plant parts were placed into the surface of potato dextrose agar (PDA) media with ampicillin (1µg/ml) as antibacterial agent. The plates were incubated at 28°C for 5-10 days. Sterile medium without plant segments was used as control to confirm the sterility of working area (El-Sayed et al., 2018). After incubation, the developed hyphal tips of the fungi were picked and purified on fresh PDA plates, incubated for 5-10 days at 28°C, and the purified fungi were stored as slant culture at 4°C (Guo et al., 2008).

Morphological and molecular identification of the recovered endophytic fungi
The purified fungal isolates were examined based on their microscopical properties according to (Raper and Fennell, 1965). The potent Taxol producing endophytic fungi were further confirmed based on their ITS rDNA sequence (El-Sayed et al., 2019)(El-Sayed et al., 2013)(El-Sayed et al., 2015). The PCR reaction contained 10µl of 2׳ PCR master mixture (i-Taq™, Cat. # 25027, iNtRON Biotech), 1µl gDNA, forward and reverse primers (10 pmol/µl) and completed to 20µl. The PCR (Thermal Cycler 006, A&E Lab Co) was programmed to initial denaturation 94°C for 2 min, 35 cycles at denaturation 94°C for 20 s, annealing 55°C for 30 s, extension 72°C for 1 min, and final extension for 5 min at 72°C. The PCR products were checked by 2% agarose gel in 1׳ TBE buffer normalizing to the DNA ladder. The amplicons were purified and sequenced using the same primer sets. The sequences were BLAST searched non-redundantly on NCBI database, and the phylogenetic tree of target sequence was constructed with MEGA 6.0 software (Tamura et al., 2011).

Chromatographic and spectroscopic analyses of extracted Taxol
The fungal cultures were grown on potato dextrose broth medium (PDB) (El-Sayed et al., 2012), after incubation of the fungal cultures, Taxol was extracted (El-Sayed et al., 2018 and 2019) and confirmed by TLC and HPLC. The extracted Taxol was analyzed by HPLC (Agilent Technology, G1315D) of C18 RP column (Eclipse Plus C18, 4.6*150mm), and methanol/ acetonitrile/water (25:35:40, v/v/v) as mobile phase, at flow rate 1 ml /min for 25 min and injection volume 20µl (Nims et al., 2006). The fractions of Taxol were scanned from 200 to 500 nm by photoiodide array detector, the concentration and identity were determined from the retention time and absorption at 227 nm.

The Taxol chemical structure of Taxol was confined by 1H NMR, 1C NMR spectra comparing to authentic Taxol (JEOL, ECA-500, 500 MHz NMR), samples were dissolved in Deuterated chloroform (CDCL3), and the chemical shifts were given in ppm with coupling constant expressed in hertz (El-Sayed et al., 2019).

The Infra-Red Spectra of extracted Taxol were analyzed using a JASCO, FTIR 6100 spectrophotometer. Samples of Taxol were ground in KBr pellets and pressed into discs by vacuum.

Nutritional optimization, and the effect of different inhibitors on Taxol yield
To investigate the optimal nutritional requirements of the potent fungi to maximize their Taxol yield, the influence of types of media in addition to the chemical inhibitors and activators were studied. The selected fungus was grown on Czapek’s-Dox media (sucrose 30 g/L, sodium nitrate 2 g/L, K2HPO4 1 g/L, MgSO4 0.5 g/L, KCl 0.5g/L, FeSO4 0.01 g/L) (Onion’s et al., 1981), Potato Dextrose Broth (PDB) (potato extract 250 g, glucose 20 g, dissolved in one liter distilled water) (El-Sayed et al., 2012), MID (El-Sayed et al., 2019), malt extract (El-Sayed et al., 2019) media.

The effect of different chemical compounds such as n-tosyl-l-phenylalanine, dinitro phenyl hydrazine, dimethylamino benzaldehyde, vitamin B12, and biotin with different concentration (10 to 200µg/ml) on taxol production by the tested fungal isolate was evaluated. The cultures were filtered to remove any mycelia and Taxol was extracted as described above. The residues were re-dissolved in methanol and analyzed by chromatographic and spectroscopic methods, as mentioned above.

Antiproliferative activity of purified fungal Taxol
The activity of extracted Taxol was evaluated against breast carcinoma (MCF7). Cells at 103-105 per well were injected into the 96-well plate, incubated for 24 hr. MTT reagent (Trevigen, Gaithersburg, USA) was added to each well, the plate was re-incubated for 2 hrs. Detergent reagent (Trevigen, Cat# 4890-25-02) was added to wells, the plate was left in dark for 4 hrs and then read at 570 nm in the plate reader. The average values of triplicates were determined and the average value for the blank was subtracted. The growth inhibition percentage was calculated using the formula percentage of cell inhibition= 100-{(At-Ab)/ (AcAb)}x100. Which, “At” is the O.D of test compound, “Ab” is O.D of blank, and “Ac” is O.D of control.

Statistical Analysis
All experiments were conducted in biological triplicates and the results were expressed by mean ±STDEV. The data were analyzed by one-way ANOVA with Fisher’s Least Significant Difference of post hoc test.


Isolation and identification of the endophytic fungal isolates
Twenty fungal isolates were isolated and recovered as endophytes inhabiting the plants Zea mays, Solanum nigrum, Portulaco oleracea, Convalvulus arrensis, Ocimum basilicum, Erchharnia crassipes, Rosa sp, Citrus xaurantium, Ricinus communis. Morphologically, the purified endophytic fungal isolates were identified according to universal keys. These fungal isolates were belonging to three genera; Aspergillus, Fusarium, Penicillium. Aspergillus represents seventeen isolates; A. flavipes (no.1), A. niger (no.5), A. terreus (no.3), A. flavus (no.7). Fusarium represented by two isolates (F. solani and F. oxysporum) and penicillium represents one isolate (P. chrysogenum) as shown in Table 1.

Table (1):
Spectroscopic and chromatographic analyses of the twenty fungal isolates.

TLC Taxol Conc.(µg/ml) Fungal isolate Host Plant Isolate No.
++ 4.92  ghi Aspergillus niger1  


Zea mays

52.12 d Aspergillus niger2 2
12.38 def Aspergillus niger3 3
24.18 fg Aspergillus niger4 4
+ 17.49 abc Aspergillus niger5  

Ricinus communis

28.8 abc Aspergillus flavipes 6
++ 120.18 a Aspergillus flavus  

Solanum nigrum

+++ 119.0 ghi Aspergillus flavus2 8
28.8 ghi Aspergillus flavus3 9
1.7 fgh Aspergillus flavus4  

Portulaco oleracea

4.7 ghi Aspergillus flavus5 11
+ 103.8 fgh Aspergillus flavus6 12
1.4 fghi Aspergillus flavus7 Convalvulus arrensis 13
33.1  fgh Aspergillus flavus 14
+++ 131.9 a Aspergillus terreus1  

Ocimum basilicum

+++ 106.2 fgh Aspergillus terreus2 16
+++ 44.2 fghi Aspergillus terreus3 Erchharnia crassipes 17
+ 36.1  fghi Fusarium oxysporum 18
+ 14.6  fghi Fusarium solani Rosa sp 19
++ 93.8  fghi Penicillium chrysogenum Citrus xaurantium 20

– Negative Taxol producer; + Mild Taxol producer; ++ Higher Taxol producer; +++ Strong Taxol producer
values given are means
– The mean values followed by different letters a, b, c with in the same column are significantly different (ONE Way ANOVA, Tukey HSD test, p≤0.05).
*** means highly significant .
-LSD: the least significant difference.

Spectroscopic and Thin layer chromatography analyses of extracted Taxol
The extracted Taxol from twenty fungal isolates was measured at wavelength 227 nm. Among these isolates, only eight fungal isolates displayed positive results, giving maximum absorption at כ227 nm, similar to authentic Taxol (Table 1). To confirm the spectroscopic assay, the samples were spotted on TLC chromatography comparing to authentic Taxol as described in Materials and Methods. The eight fungal isolates namely A. flavipes, A.flavus1, A. flavus 2, A. flavus 6, A. terreus 1, A. terreus 2, A. terreus 3, P. chrysogenum showed distinct spot under UV illumination at 254 nm with Rf value 0.7 which was identical to authentic taxol as showed in Fig. 1, with bluish spot when TLC sheets sprayed with vanillin/ sulphuric acid reagent. From these fungal isolates, A. terreus 1 displayed the highest yield of Taxol (131.7µg/ml) and the potent taxol spot.

Fig. 1. Screening for Taxol producing potency among the recovered endophytic fungi.

HPLC, NMR and IR analyses of extracted Taxol
To investigate the presence of Taxol, fungal Taxol and authentic Taxol were subjected to HPLC analysis where authentic Taxol gave a peak with a retention time 1.8 min similar to fungal Taxol which gave a peak with retention time 1.89 min (Fig. 2). For further confirmation of the chemical structure of Taxol, the 1H NMR analysis was performed where the signals of 1H NMR for the fungal extract was found to be consistent to the authentic taxol, the signals were distributed at 1.0 and 8.0 ppm. The proton signals appeared in the region between 1.0 and 2.5 ppm matching to methyl, acetate and acetylene groups (Kumaran et al., 2008; El-Sayed et al., 2019). Signals of most of protons in the taxane skeleton and their side chains protons were appeared in the region between 2.0 and 7.0 ppm while the signals for aromatic moieties corresponding to the benzoate (2-OCOph), phenyl (C3′-ph) and benzamide (3’NH-COph) groups were determined at 7.0 and 8.4 ppm (Chmurny et al., 1992; Zhang et al., 2009; Strobel et al., 1996).

Fig. 2. Chromatographic and Spectral analyses of the extracted Taxol from A. terreus. HPLC chromatogram of authentic Taxol. (A), A. terreus extracted Taxol (B). NMR spectrum (C) and FT-IR spectrum (D) of A. terreus Taxol.

FT-IR analysis, Taxol of A. terreus displayed similar FT-IR peaks of standard Taxol as shown in Fig. 2. The peaks at 3406 and 3393 cm-1 were assigned for hydroxyl (OH) and amide (±C (O) NH±) groups stretch (Kumaran et al., 2008). However, the peaks at 2923, 1729 and 1604 cm-1 were assigned to the aliphatic CH stretch, ester groups stretch and aromatic rings stretch (Das et al., 2017). The COO stretching frequency was peaked at 1268 cm-1, while the peak at 1029 cm-1 was allocated for the aromatic C, H bends.

Nutritional optimization of Aspergillus terreus to maximize their Taxol yield
Different types of media
Aspergillus terreus was cultivated on different media (PDB, MID, DOX, Malt extract). From the obtained results (Fig. 3), A. terreus gave the highest Taxol yield by growing on PDB media (132µg/ml) followed by malt extract media (128.47µg/ml), with distinct corresponding Taxol spots on the TLC plates. However, the yield of Taxol by A. terreus was significantly low, with undetectable spots on TLC plates, under the standard conditions by growing on Czapek’s-Dox and MID media. Consistently, PDB supports the maximum Taxol yield by A. terreus (El-Sayed et al., 2018b) and A. flavipes (El-Sayed et al., 2019a).

Fig. 3. Taxol yield of A. terreus by growing on different types of media and in response to different growth inhibitors. A, The fungal isolate was grown on different potato dextrose broth, malt extract, Czapek’s-Dox and MID media (El-Sayed et al, 2018), and the Taxol was extracted and determined by HPLC. The cultures of A. terreus were amended with different inhibitors, incubated at standard conditions, then Taxol was extracted and quantified (B) from HPLC chromatogram (C).

Different chemical compounds
The effect of various inhibitors such as N-p-tosyl-l-phenylalanine, dinitrophenyl-hydrazine, dimethyl amino benzaldehyde, vitamin B12, Biotin at different concentration (10, 50, 100, 150, 200µg/ml) on Taxol production by A. terreus was evaluated. The fungal cultures were cultivated with each compound on PDB medium for 15 days at 28°C, then the Taxol yield was determined. From the results of UV spectroscopy and TLC chromatography, the Taxol yield by A. terreus in presence of biotin (150µg/ml), vitamin B12 (150µg/ml) and dinitrophenyl-hydrazine (100µg/ml) was significantly increased by about 3.5, 3.5 and 4.1 folds, respectively, comparing to control (Table 2), with p value was < 0.0001. Thus, among the tested compounds, biotin displayed a significant inducing activity on Taxol yield by A. terreus by about 4.1 folds. The Taxol yield by A. terreus was slightly increased in presence of vitamin B12, dimethylamino benzaldehyde and dinitrophenyl hydrazine at 10µg/ml comparing to control. The taxol yield by A. terreus in response to these inhibitors was authenticated from the HPLC analysis (Fig. 4). From the obtained results, the Taxol yield by A. terreus was maximally increased by incorporation of biotin, vitamin B12, and dinitrophenylhydrazine by 5, 2.2 and 1.6 folds, respectively, comparing to control.

Fig. 4. Antiproliferative activity of extracted Taxol from A. terreus towards MCF-7 breast cell lines in vitro.

Table (2):
Effect of different chemical compounds on Taxol yield by A. terreus.

Compound Conc.
Taxol conc. (µg/ml) TLC Increasing fold
Control 0 163.9±9.6 ghi


N-tosyl-L-phenyl alanine

10 286.9±34 efgh + 1.7
50 215.7±5.6 fghi + 1.3
100 331.8±1.7 def + 2
150 162.3±3.7 hi
200 318.5±2.4 ef + 1.94


Dinitrophenyl hydrazine

10 375.8±11.6 cde + 2.29
50 307.6±75.2 efg + 1.87
100 605.6±2.8 ab +++ 3.6
150 471.5±2.5 bcd ++ 2.8
200 128.1±8.4 i


Dimethyl amino benzaldehyde

10 376.6±8.9 cde + 2.29
50 570.8±42.6 ab ++ 3.48
100 514.2±7.5 bc ++ 3.13
150 341.4±7.4 def + 2.08
200 320.9±6.4 ef + 1.95


Vitamin B12

10 379.7±71.2 cde 2.3
50 571.8±90.5 ab ++ 4.17
100 510.5±95.5 bc ++ 3.11
150 343.4±11.61 def + 2.8
200 325.8±68.9 ef + 1.98




10 361.6±63.5 de + 2.2
50 347.6±85.9 def + 2.2
100 410.8±22.9 cde ++ 2.5
150 663.8±0.57 a +++ 4.04
200 476.7±76.8 bcd +++ 2.9
P ***(0.0000)
LSD 0.05 74.88

-values given are means
– The mean values followed by different letters a, b, c with in the same column are significantly different (ONE Way ANOVA, Tukey HSD test, p≤0.05).
*** means highly significant .
-LSD: the least significant difference.

Antiproliferative activity using MTT test
The antiproliferative activity of A. terreus Taxol was evaluated against MCF7-E (breast cancer cell). The IC50 value of A. terreus Taxol was 0.3 ng/ml towards MCF7-E (Fig. 4). The activity of extracted Taxol was noticed to be a dose-dependent manner towards the tested cell line. Coincident results authenticating the antiproliferative activity of A. terreus Taxol was documented in our previous studies (El-Sayed et al., 2019c; El-Sayed et al., 2018a and Zein et al., 2019).


Aspergillus terreus an endophyte of Ocimum basilicum displayed the highest potency for Taxol production, among the recovered endophytic fungal isolates from different medicinal plants. The yield of Taxol from A. terreus has been increased by about 4 folds upon addition of biotin at 150µg/ml to the culture media after 5 days of cultural pre-incubation. The chemical identity of the extracted Taxol was validated by HPLC and spectroscopic analysis, as well as their anticancer activity was emphasized towards the MCF-7, regarding to authentic Taxol.


We appreciate the partial financial support from Zagazig University, and facilities at Enzymology and Fungal Biotechnology Lab, at Faculty of Science, Zagazig University, Egypt.

The authors declare that there is no conflict of interest.

ASAE and AEH designed and wrote the manuscript; MTE and HSN revise and edit the manuscript, EKY perform the experiments.

We appreciate the partial financial support (Grant # EBFL2018019) from Botany and Microbiology Department, Faculty of Science, Zagazig University, Egypt.

The study was conducted ethically in accordance with the World Medical Association Declaration of Helsinki.

The raw data required to reproduce these findings are available to download from

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