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Article

Purification and Biochemical Characterization of Taxadiene Synthase from Bacillus koreensis and Stenotrophomonas maltophilia

by
Ashraf S. A. El-Sayed
1,*,
Maher Fathalla
2,3,
Ahmed A. Shindia
1,
Amgad M. Rady
4,
Ashraf F. El-Baz
5,
Yara Morsy
2,
Basel Sitohy
6,7 and
Mahmoud Sitohy
8
1
Enzymology and Fungal Biotechnology Lab (EFBL), Botany and Microbiology Department, Faculty of Science, Zagazig University, Zagazig 44519, Egypt
2
Chemistry Department, Faculty of Science, Zagazig University, Zagazig 44519, Egypt
3
Department of Chemistry, Faculty of Science, Islamic University of Madinah, Madinah 42351, Saudi Arabia
4
Faculty of Biotechnology, October University for Modern Sciences and Arts, Cairo 12585, Egypt
5
Genetic Engineering and Biotechnology Research Institute (GEBRI), University of Sadat City, Sadat City 32897, Egypt
6
Department of Clinical Microbiology, Infection and Immunology, Umeå University, SE-90185 Umeå, Sweden
7
Department of Radiation Sciences, Oncology, Umeå University, SE-90185 Umeå, Sweden
8
Biochemistry Department, Faculty of Agriculture, Zagazig University, Zagazig 44519, Egypt
*
Author to whom correspondence should be addressed.
Sci. Pharm. 2021, 89(4), 48; https://doi.org/10.3390/scipharm89040048
Submission received: 16 September 2021 / Revised: 18 October 2021 / Accepted: 21 October 2021 / Published: 9 November 2021
Browse Figures
Versions Notes

Abstract

:
Taxadiene synthase (TDS) is the rate-limiting enzyme of Taxol biosynthesis that cyclizes the geranylgeranyl pyrophosphate into taxadiene. Attenuating Taxol productivity by fungi is the main challenge impeding its industrial application; it is possible that silencing the expression of TDS is the most noticeable genomic feature associated with Taxol-biosynthetic abolishing in fungi. As such, the characterization of TDS with unique biochemical properties and autonomous expression that is independent of transcriptional factors from the host is the main challenge. Thus, the objective of this study was to kinetically characterize TDS from endophytic bacteria isolated from different plants harboring Taxol-producing endophytic fungi. Among the recovered 23 isolates, Bacillus koreensis and Stenotrophomonas maltophilia achieved the highest TDS activity. Upon using the Plackett–Burman design, the TDS productivity achieved by B. koreensis (18.1 µmol/mg/min) and S. maltophilia (14.6 µmol/mg/min) increased by ~2.2-fold over the control. The enzyme was purified by gel-filtration and ion-exchange chromatography with ~15 overall folds and with molecular subunit structure 65 and 80 kDa from B. koreensis and S. maltophilia, respectively. The chemical identity of taxadiene was authenticated from the GC-MS analyses, which provided the same mass fragmentation pattern of authentic taxadiene. The tds gene was screened by PCR with nested primers of the conservative active site domains, and the amplicons were sequenced, displaying a higher similarity with tds from T. baccata and T. brevifolia. The highest TDS activity by both bacterial isolates was recorded at 37–40 °C. The Apo-TDSs retained ~50% of its initial holoenzyme activities, ensuring their metalloproteinic identity. The activity of purified TDS was completely restored upon the addition of Mg2+, confirming the identity of Mg2+ as a cofactor. The TDS activity was dramatically reduced upon the addition of DTNB and MBTH, ensuring the implementation of cysteine-reactive thiols and ammonia groups on their active site domains. This is the first report exploring the autonomous robust expression TDS from B. koreensis and S. maltophilia with a higher affinity to cyclize GGPP into taxadiene, which could be a novel platform for taxadiene production as intermediary metabolites of Taxol biosynthesis.

1. Introduction

Taxol is one of the most traded, powerful antimitotic drugs and can cause cellular arrest during the G2/M phase of various tumor cells, including in leukemia, breast, ovarian, and lung cancer cells [1]. Taxadiene synthase (TDS) is a type I diterpene cyclase that catalyzes the first committed step of Taxol biosynthesis by cyclizing the geranylgeranyl pyrophosphate generating tricyclic hydrocarbon skeleton of Taxol “taxadiene” [2,3,4]. Taxadiene synthase, the biochemistry of Taxol biosynthesis, and different strategies for commercial Taxol production from endophytic fungi and plants have been extensively reviewed [5,6,7,8,9,10]. The emergence of endophytic fungi as a source of Taxol is a promising new avenue for commercial Taxol production due to their fast growth, cost effectiveness, independence from climatic changes, and feasibility of genetic manipulation [11,12,13]. Taxomyces andreanae was the first reported Taxol producer endophyte from Taxus spp. [2], followed by a plethora of endophytic fungi with Taxol producing potency from the Taxus species and other related plants [5,6,9,10,14,15,16,17,18]. Unfortunately, the exploitation of fungi as an industrial platform for Taxol production has been challenged by the loss of Taxol productivity due to fungal storage and subculturing [11,12]. Aspergillus flavipes and A. terreus, endophytes of Podocarpus gracilior, have been recognized as efficient Taxol producers for the initial cultures; however, their Taxol biosynthetic potency is strongly attenuated by subculturing and storage [5,10,14,15,16,17,18]. Several strategies have been proposed to restore the biosynthetic machineries of Taxol via fungi, such as the implementation of sterilized plant parts with the entire microbiome, which was able to dramatically restore the biosynthetic machinery of Taxol [5,10,16], as well as cocultivation with the bacteria Bacillus subtilis, which had a significant effect on the Taxol biosynthetic machinery of A. flavipes [19]. Taxol productivity by A. flavipes was completely restored upon cocultivation with Bacillus subtilis due to the production of specific chromatin remodeling signals that triggered the expression of the fungal biosynthetic genetic cluster of Taxol [9,16,19].
Downregulating the expression of the taxadiene synthase and the subsequent reduction on the cellular flux of taxadiene are the plausible metabolic traits that are associated with the attenuation of the Taxol biosynthetic machinery of fungi [9,16]. There are two types of diterpene cyclases: type I exhibits a single domain (a-domain) with the active sites of conserved motifs, including aspartate-rich motif DDXX(X)(D,E) and the NSE triad ND(L,I,V)XS XXXE, which are mainly involved in binding the Mg2+ cofactor and form a trinuclear cluster for binding with the substrate diphosphate unit [20,21]. Type II shares a highly conserved DXDD motif for the protonation of the substrate [22]. Type I utilizes a trinuclear metal cluster to trigger the ionization of the isoprenoid diphosphate substrate to yield allylic cation and inorganic pyrophosphate [23]. The initial GGPP cyclization probabilities are determined via metal-dependent ionization and the departure of the diphosphate group between the first carbon atom and one of the following carbon atoms: C6, C7, C10, C11, C14, and C15, creating bond-forming reactions [23,24]. Terpenoids are categorized based on the type of carbon–carbon interaction during the initial GGPP cyclization reaction: C1–C11 (cyclooctatenol synthase), C3–C8 (entkaurene synthase), C1–C14 (taxadiene synthase), and putative labdane-related diterpene cyclase (LrdC) [23].
Given the high demand for Taxol in cancer chemotherapy, metabolic engineering approaches for the overproduction of taxadiene intermediates is one of the most recognized approaches. Several metabolically engineered microbes that can produce taxadiene have been reported, such as Escherichia coli [25] and Saccharomyces cerevisiae [26], which are dependent on the cloning of the TDS gene from T. baccata [27]. However, there are no reports describing the natural/wild presence of TDS in bacteria with autonomous expression that is independent of external signals from plant hosts; thus, searching for autonomously TDS producing bacteria as well as for methods for the the purification, biochemical, and kinetic characterization of this enzyme is the objective of this study.

2. Materials and Methods

2.1. Materials

Geranylgeranyl pyrophosphate (Cat. # G6025) and polyacrylamide solution were purchased from Sigma-Aldrich Co. (Saint Louis, MO, USA). Sephadex G200 and DEAE-Sepharose were obtained from Pharmacia Co. Protein ladder (Blue Plus Maker, Cat. # DM101, 14–100 kDa) was obtained from ThermoFisher Scientific, Massachusetts, USA. All other chemicals were of analytical grade.

2.1.1. Isolation and Screening for TDS Producing Endophytic Bacteria from Different Plants

Different plants, namely Mentha x piperita L., Coriandrum sativum L., Anethum graveolens L., and Moringa oleifera Lam., were collected from Zagazig, Alsharqia province, Egypt. Parts of the leaves and twigs of Podocarpus gracilior were collected from the Orman Botanical Garden, Cairo, Egypt, were washed thoroughly with sterile distilled water, and were sectioned into small parts. These parts were surface sterilized with 70% ethyl alcohol for 1 min and 2.5% sodium hypochlorite for 2 min and were rinsed with sterile distilled water to avoid any epiphytic microbial flora [28,29,30]. These sections were aseptically cultured on different solid media in plates containing potato dextrose agar (PDB, Difco), beef–yeast extract glucose (0.15% beef extract, 0.3% yeast extract, 0.1% glucose, 0.6% peptone), and nutrient agar (0.2% yeast extract, 0.5% peptone and 0.5% NaCl) and were incubated at 30 °C. The plates were incubated for 5 days, and the actively growing microbial colonies were selected and sub-cultured on the corresponding media. The selected bacterial colonies were eventually grown on Luria–Bertani (LB) medium (LB Broth Miller, Molecular Genetics, Granular) and were stored in 25% glycerol at −20 °C.
The metabolic producing potency of TDS by the recovered bacterial isolates was evaluated through growth on nutrient broth media [29]; An amount of 1 ml of each bacterial spore suspension (103 CFU/mL) was inoculated into 50 mL media/250 mL Erlenmeyer conical flask and incubated at 30 °C for 4 days at 120 rpm. The bacterial cultures were pelleted by centrifugation at 8000 rpm for 10 min, the pellets (1 g) were washed, pulverized in liquid nitrogen, and dispensed in 5 mL HEPES buffer (30 mM, pH 8.0) with 5 mM sodium ascorbate, 5 mM DTT, 1 mM PMSF, 5 mM Na2S2O5, 15 mM MgCl2, 10% (v/v) glycerol, and 1% (w/v) polyvinylpolypyrrolidone [3,16,17,31]. The mixtures were shacked thoroughly and centrifuged at 8000 rpm for 15 min, and the supernatant was used as the source of the crude enzyme. Triplicates from each bacterial isolate were conducted, and the TDS activity was represented by the average. The activity of the crude TDS and the protein concentration were estimated described as below.

2.1.2. Taxadiene Synthase Activity and Protein Concentration

The TDS activity was determined according to the method proposed by Hezari et al. [3], with minor modifications [6,9,15]. Briefly, the reaction mixture contained 50 mM geranylgeranyl pyrophosphate (GGPP), 5 mM MgCl2 in 50 mM Tris-HCl pH 8.0, and 500 μL enzyme extract of each bacterial isolate in a 2 mL total reaction volume. The reaction mixture was incubated at 37 °C for 30 min, which was stopped by 500 μL EDTA (0.5 M, pH 8.0). The GGPP concentration was determined by TLC with 60 F254 silica gel plates (Merck KGaA, Darm. Germany) with the developing solvent system, which comprised propanol, ammonia, and water (9:3:1) for the authentic GGPP (Cat. # G6025). After running the solvent, the TLC plates were visualized using vapor iodine [32]. The intensities of the GGPP spots were determined using the Image J software package [33]. One unit of TDS activity was expressed by the amount of enzyme consuming 1 μmol of GGPP per min under the standard assay conditions.
The protein concentration used for the enzyme preparation was determined by Bradford’s reagent using bovine serum albumin as the standard [34].

2.1.3. Chemical Identity of Taxadiene

The putative spots of the TDS byproducts were scraped-off of the silica, eluted by dichloromethane, and analyzed by gas chromatography-tandem mass spectrometry [17,30,35]. The chemical identity of the resolved putative taxadiene from the TDS activity of selected samples was resolved by GC-MS/MS (Agilent Technologies 7890A) interfaced with a mass-selective detector (MSD, Agilent 7000) equipped with a polar Agilent HP-5 ms (5%-phenylmethyl poly siloxane) capillary column (30 m × 0.25 mm). The sample was injected 1 μL with helium as a carrier gas, and the linear velocity was 1 mL/min. The MS operating parameters had an ionization potential of 70 eV, an interface temperature 250 °C, and a mass acquisition range of 50–800. The chemical identity of the putative taxadiene was determined by relying on the comparison of their mass spectra and their fragmentation patterns using the NIST and WILEY libraries in addition to the fragmentation patterns of the mass spectral data of the authentic compound. The name, molecular weight, and structure of the components of the tested material were ascertained.

2.1.4. Molecular Detection of TDS by PCR

To confirm the spectroscopic and chromatographic activity of TDS, s molecular validation of the tds genes was conducted by means of PCR using bacterial DNA as a template [29]. Bacterial DNA were extracted with CTAB reagent [30,36], which was used as the PCR template with the primer set tds1 5′-GCAGCGCTGAAGATGAATGC-3′, 5′-CGATTCGATACCCCACGATCC-3′ and tds2 5′-ATGTCCAAACCCATGTCGAA-3′, and 5-ACCCATGTCGAATTGAGAAGAT-3′. The PCR reaction mixture contained 10 μL of 2× PCR master mixture (i-TaqTm, Cat. #25027, iNTRON Biotech), 2 μL of gDNA, and 1 μL of the forward and reverse primers (10 pmol/μL); the reaction was completed by adding sterile distilled water until a volume of 20 μL was reached. PCR amplification was performed using a Thermal Cycler 006 (A&E Lab Co., Ltd., London, England), which was programmed for initial denaturation at 94 °C for 2 min, denaturation at 94 °C for 20 s, annealing at 53–55 °C for 30 s, extension at 72 °C for 1 min for 35 cycles, and final extension for 2 min at 72 °C. The PCR products were analyzed using 1.5% agarose gel, and the PCR amplicons were purified and sequenced using the same primer sets.

2.1.5. Molecular Identification of the Potent TDS Producing Bacterial Isolates

Potent TDS producing bacteria were identified based on their 16S rDNA sequence [29,33] using the universal primer set 5′-AGAGTTTGATYMTGGCTCAG-3′ and 5′-CAKAAAGGAGGTGATCC-3′. A loopful of actively growing bacterial colonies were suspended in 50 μL lysis buffer (10 mM Tris-HCl, 50 mM KCl and 0.1% Tween 20 (pH 8.3), and they were incubated at 99 °C for 10 min. A 1 μL aliquot of the bacterial lysate was used as a template for the PCR amplification of the 16S rDNA gene. The PCR reaction contained 10 μL of 2× PCR master mixture (Cat. #. 25027), 2 μL of bacterial lysate, and 1 μL of forward and reverse primers (10 pmol/μL), and the solution was completed with the addition of sterile distilled water up to a volume of to 20 μL. The PCR was programmed for initial denaturation at 94 °C for 2 min, 38 cycles with denaturation at 94 °C for 30 s, annealing at 55 °C for 10 s, extension at 72 °C for 30 s, and a final extension at 72 °C for 2 min. The amplicons were analyzed using 1.5% agarose gel in 1× TBE buffer with a DNA ladder and were sequenced using the Applied Biosystems Sequencer, HiSQV Bases, Version 6.0 with the same primer sets. The sequences were BLAST searched non-redundantly on the NCBI database and were aligned with the ClustalW muscle algorithm [37]; the phylogenetic tree was constructed using a neighbor-joining method with 1000 bootstrap replications [38].

2.1.6. Bioprocess Optimization of the Potent Bacterial Isolates for Maximizing Their TDS Yield by Two-Factorial Plackett-Burman Design and Faced Central Composite Design (FCCD)

The selected physicochemical properties, namely yeast extract, peptone, phenylalanine, tyrosine, tryptophan, glycine, valine, methionine, asparagine, cysteine, glutamic acid, beef extract, sucrose, glucose, xylose, NaCl, ammonium nitrate, incubation time, and pH were optimized using a two factorial Plackett–Burman design to identify the significant variable affecting TDS production [35,39]. The nineteen variables were optimized using the Plackett–Burman design. Each variable was represented by high (+) and low (−) levels. The Placket–Burman design depends on the first order reaction:
Y = βo + Σβ1X1
where Y is the predicted terpene cyclase production, Xi is an independent variable, βi is the linear coefficient, and β0 is the model intercept. All of the runs were conducted in triplicate, and the average of terpene cyclase production was used as a response.
The most significant positive independent variables affecting TDS production by the selected bacteria were optimized using FCCD to determine the individual and mutual interactions of the tested variables. In the FCCD experimental design, each variable was represented by three different levels, low (−1), medium (0), and high (+1), and the center point was repeated six times, resulting in a total 20 runs.

2.1.7. Purification and Molecular Subunit Structure of TDS from the Most Potent Bacteria

The potent TDS producing bacteria were grown on the optimized enzyme production media from the surface response methodology using different factorial designs. After incubation, the bacterial pellets (~50 g) were collected, washed with sterile potassium phosphate buffer (50 mM, pH 7.0), pulverized in liquid nitrogen, and dispensed in 50 mL of HEPES buffer comprising 1 mM ethylenediaminetetra acetic acid (EDTA), 1 mM phenylmethansulphonylfloride (PMSF), 1 mM β-mercaptoethanol, and 1 mM CaCl2 [8,40,41,42,43]. After homogenization, the mixture was vigorously agitated for 15 min and was then centrifuged at 8000 rpm for 10 min to remove the cell debris. The supernatant was used as source of crude enzymes. The activity and protein content of crude enzyme were measured as above. The crude proteins were precipitated by two volumes of child acetone for 15 min at −20 °C, the precipitated proteins were collected by centrifugation at 10,000× g for 5 min, and the protein pellets were dissolved in 50 mL HEPES buffer (pH 7.4, 50 mM) [8]. The precipitated proteins were fractionally concentrated with 20 kDa cut-off dialyzer (Cat. # 546-00051) against polyethylene glycol 6000 until the minimum volume was reached (5 mL). The enzyme was purified by means of the gel-filtration and ion-exchange chromatographic approaches [18,19,20,21,22,23,24,25,26,27,28,29,30,31,32,33,34,35,36,37,38,39,40,41,42,43]. The crude protein (2 mg) was loaded into the column of Sephadex-G200 (2 × 40 cm) and was pre-equilibrated with 50 mM potassium phosphate buffer (pH 7.5) at flow rate 0.5 mL/min. The enzyme fractions (1 mL) were eluted with the same buffer, and their activity and concentrations were determined by the standard assay. The most active, molecularly homogenous fractions were collected and were concentrated by means of dialysis against polyethylene glycol 6000. The partially purified enzymes from the first step were further purified by ion-exchange chromatography using a DEAE-Sepharose column (2 × 30 cm) that had been preequilibrated with potassium phosphate buffer (0.1 mM, pH 7.5). The sample (1 mg) was loaded on to the top of the column, and after gel-permeation, the column was equilibrated with the same buffer at a flow rate 0.5 mL/min. The enzyme was eluted by gradient NaCl concentrations (100–300 mM) with the same buffer. The activity and protein content of the obtained fractions were determined by the above assay. The most active and homogenous TDS fractions were collected and were concentrated with 10 K ultra-centrifugal membrane and were stored at 4 °C for further analysis.
The molecular homogeneity and subunit structure of purified TDS were checked using SDS-PAGE [44] with slight modifications [43,45,46]. The molecular mass of the purified TDS was determined and was normalized to an authentic protein marker (Puregene, Cat. # PG-PMT2962 315–10 kDa). The entire molecular mass of the purified TDS was determined by native-PAGE [44].

2.1.8. Biochemical Properties of the Purified TDS from the Potent Bacterial Isolate

The most active and molecular homogenous fractions were gathered for subsequent biochemical characterization [8,40,41,42,47,48,49]. The optimum reaction temperature for the TDS activity was evaluated by incubating the enzymatic reaction at 4, 20, 30, 37, and 45 °C, measuring the enzyme activity using the standard assay. The thermal stability was assessed by pre-incubating the enzymes without substrate at 4, 20, 37, 45 and 50 °C, at 15, 30, 60 and 180 and 240 min, and then measuring their residual activities with the standard assay. The thermal kinetic parameters half-life time (T1/2), half-life temperature (Tm), and thermal inactivation rate (Kr) were determined [48].
The effect of the reaction pH (3.0–10.0) on the activity of the purified TDS were investigated using 50 mM of citrate phosphate buffer (pH 3.0–5.0) and Tris−HCl (6.0–10.0). The pH stability was evaluated by preincubating the enzyme at different pHs for 2 h at 4 °C and then measuring their residual activities by standard assay as described above. The effect of different inhibitors on the activity of the TDS activity was assessed. The purified enzyme preparations were desalted by dialysis (Cat. # 546-00051, Wako Chem., Richmond, VA, USA) against 50 mM Tris-HCl buffer (pH 8.0) of 1 mM EDTA. Different cations, namely Ba2+, Fe3+, Ca2+, Hg2+, Fe3+, Al3+, Zn2+, Na+, and Cu2+ were added to the enzymes at a final concentration of 1 mM, incubated for 2 h at 4 °C, and the substrate was then added, with the enzyme activity being measured by the standard assay. The influence of suicide amino acid reactive analogues, namely hydroxylamine, iodoacetate, guanidine thiocyanate, DTNB, and MBTH (1 mM final conc.), on the activity of the purified TDS was assessed. The mixtures were incubated for 2 h at 4 °C, and then the residual activities of the enzymes were measured by the same standard assay as the one described before.
Statistical analysis: All of the experiments were conducted in biological triplicates, and the results were expressed by mean ± STDEV. The significance and F-test were calculated using one-way ANOVA with Fisher’s least significant difference post hoc test.

3. Results

3.1. Screening for the Potent Taxadiene Synthase Producing Bacterial Isolates

Twenty-three endophytic bacterial isolates were recovered from the surface of sterilized leaves of Mentha x piperita L., Coriandrum sativum L., Anethum graveolens L., Moringa oleifera Lam., and P. gracilior on the media PDA, beef–yeast extracts glucose, and nutrient agar (Table S1). These bacterial isolates were purified and stored on nutrient agar media. The TDS producing potency of the recovered bacterial isolates were assessed by being grown on PDB for 4 days at 30 °C, and the cultures were pelleted and pulverized in liquid nitrogen, and the intracellular proteins were extracted, and the enzyme activity and concentrations were determined by the standard assay. Among the recovered bacterial isolates, seven bacterial isolates, # 10, 37, 38, 39, 40, 41, and 42, displayed the highest potency for TDS production (Figure 1). The highest TDS activity was produced by bacterial isolate # 41 (8.8 µmol/mg/min), followed by isolate # 42 (4.7 µmol/mg/min), while TDS production ranged between 1.9–2.6 µmol/mg/min for bacterial isolates # 10, 37, 38, 39, and 40. Interestingly, the highest TDS-producing bacterial isolates (#41, 42) were isolated as endophytes of P. gracilior, which is the host of the Taxol-producing endophytic fungal isolate A. terreus [9,18]. The TDS activity was clearly revealed from the residual concentration of GGPP on the TLC chromatogram, as shown on Figure 1 (upper panel). The biosynthetic potency of TDS was confirmed from the nested-PCR detection of the tds genes that were designed based on the conserved active sites sequences of the TDS from different fungal and plant sources. The metabolic producing potency of TDS by isolates 41 and 42 was confirmed from the positive PCR amplicons from the specific active site-designed tds primers (Figure 1C,D) compared to the negative TDS-producing bacterial isolates. The amplicons of tds1 were about 500 bp for bacterial isolates # 41 and 42, while the tds2 amplicons were approximately 300 bp for both bacterial isolates, and there was an absence of PCR amplicons for the negative enzyme-producing isolates.
The chemical identity of the released taxadiene as the byproduct of TDS activity was verified by GC-MS analysis. The enzymatic reaction of the putative crude TDS and GGPP as a substrate in HEPES buffer was incubated for 15 min at 30 °C, then the reaction mixture was spotted on TLC, and the developed plates were visualized by vapor iodine. The developed putative taxadiene spots were scarped-off and were analyzed by GC-MS. From the GC-MS profile (Figure 2), the fragmentation pattern of the parent and daughter molecules of the putative taxadiene samples was coincident to the authentic one. The molecular mass of the parent taxadiene molecule was 271.2 m/z compared to the authentic taxadiene molecule, which was 272.1 m/z [3,27]. The fragmentation pattern of the parent taxadiene molecule as byproduct of putative TDS from bacterial isolate # 41 generated common daughter ions of 57.1, 81, 95, 107, 122, 147.1, and 197.1, which is consistent with the fragmentation pattern of authentic taxadiene [27].

3.2. Molecular Identification of the Potent TDS Producing Bacterial Isolates (# 41 and 42)

The potent TDS-producing bacterial isolates # 41 and 42 were molecularly identified based on the sequence of their 16 S RNA region. Using the gDNA of these bacteria as a template for PCR, the size of the resolved amplicons ranged from 550–600 bp (Figure 3). These 16 S amplicons were purified and sequenced, and any that were non-redundant were BLAST searched in the NCBI database. Bacterial isolates # 41 and 42 were identified as Bacillus koreensis and Stenotrophomonas maltophilia, and their 16S RNA sequences were deposited in the NCBI database with accession # MN592666.1 and MN592660.1, respectively. From the alignment, applying the Neighbor-Join and BioNJ algorithm with the maximum composite likelihood approach, the phylogenetic relatedness of these sequences was constructed. Bacillus koreensis EFBL MN592666.1 displayed a 99% similarity with the database-deposited isolates of B. koreensis MT102961, NR116851, MF151752, FJ389509.1, MH801097.1, MT214157.1, JQ026323.1, JN578481.1, GQ302985.1, and KC894754.1, with an E-value zero and a query coverage of 98%. Stenotrophomonas maltophilia EFBL MN592660.1 had a 98% similarity with the database-deposited S. maltophilia KP82608.2, KP165415.1, EU931549.1, JF711013.1, KC136828.1, FN645734.1, FR823396.1, MN192109.1, AJ131907.1, KT580665.1, KX817899.1, KF668478.1, KT580654.1, and KF463870.1, with an E-value zero and a query coverage of 96%.

3.3. Bioprocess Optimization of TDS Productivity of B. koreensis and S. maltophilia by Response Surface Methodology

Nineteen independent variables, namely yeast extract, peptone, phenylalanine, tyrosine, tryptophan, glycine, valine, methionine, asparagine, cysteine, glutamic acid, beef extract, sucrose, glucose, xylose, NaCl, ammonium nitrate, incubation time, and pH, were screened for TDS productivity by the potent bacteria isolates using a Plackett–Burman design (Table 1). The matrix of the Plackett–Burman design with the significance of the independent variables affecting TDS productivity by B. koreensis with the predicted and actual values shown in Table 2. The fluctuation of the predicted TDS yield that had been resolved from the Plackett–Burman design ranged from 2.2 to 18.0 µmol/mg/min, reflecting the significance of the optimization process and the efficiency of the Plackett–Burman design. The maximum TDS actual activity by B. koreensis (18 µmol/mg/min) was obtained in the presence sucrose (1 g), peptone (5 g), ammonium nitrate (4 g), tryptophan (1 g), tyrosine (1 g), glucose (1 g), glutamic acid (1 g), glycine (1 g), and methionine (4 g) per liter of distilled water, at a pH 6.0, and after 6 days of icubation.
The correlation between TDS productivity by B. koreensis and the independent variables was assessed through the multiple-regression statistical analysis of variance (ANOVA) of the experimental design. The significance of the tested variables on the production of TDS by the bacterial isolate was clearly shown with a Pareto Chart, a probability plot of the independent variables, which showed the actual and predicted TDS productivity (Figure S1). The significance of each coefficient was determined from the p-value and student’s t-test. From the normal probability plot, the points of the residuals were arranged near the diagonal line, revealing the independent normal distribution of the variables, ensuring the perfect fitting of the expected TDS productivity. From the ANOVA analysis of the Plackett–Burman design, the constructed model was highly significant, which was revealed values of Fisher’s F-test value of 7.4 and the lower probability p-value of 0.029. Thus, upon using the Plackett–Burman design, the TDS productivity of B. koreensis increased from 8.8 to 18.1 µmol/mg/min, i.e., a 2.1-fold increase.

3.4. Purification, and Molecular Subunit Structure of TDS from S. maltophilia and B. koreensis

Taxadiene synthase was purified from the potent bacterial isolates S. maltophilia and B. koreensis, which were grown on the nutritionally optimized medium from the response surface methodology designs. After incubation, the bacteria cells were pelleted, and the intracellular proteins were extracted, and the TDS was purified by the size-exclusion and ion-exchange chromatographic approaches [40,41,42,47]. The protein fractions were eluted from the columns, and the TDS activity and concentration were determined by the standard assay. Apparently, the active TDS fractions from both chromatographic approaches displayed relative proximity in terms of their molecular mass and overall charge (Figure 4). The overall purification profile of both of the bacterial isolates is shown in Table 3. When the gel-filtration step was used, the TDS activity from B. koreensis and S. maltophilia increased by 2.9- and 10.6-fold, while when using ion-exchange chromatography, the enzyme activity increased by about 15.9- and 14.6-fold, respectively. By the last purification, the specific activity of the purified TDS in B. koreensis and S. maltophilia was 6.84 µmol/mg /min and 1.7 µmol/mg/min, respectively. The overall purification yields of TDS from both of the bacterial isolates were 19.2 and 16.9%, respectively.
The molecular homogeneity of the active TDS fractions was checked, and the most homogenous molecular fractions were gathered and concentrated prior to the next purification step. The entire molecular mass and molecular subunit structures of the purified TDS from both bacterial isolates were determined from the native-PAGE and SDS-PAGE analyses (Figure 4). From the native-PAGE, the entire molecular mass of the purified TDS from both of the bacterial isolates displayed approximately 180 kDa. Under denaturing conditions, the purified TDS from B. koreensis and S. maltophilia were recorded to be 65 and 80 kDa, respectively. From the native and SDS-PAGE, the purified TDS from the bacterial isolates had two identical subunits, meaning that it had a homodimeric identity.

3.5. The Biochemical Properties of Purified TDS from Both Bacterial Isolates

The biochemical properties of the purified TDS from B. koreensis and S. maltophilia such as reaction temperature, thermal stability, reaction pH, and pH stability were determined. The influence of the reaction temperature on the TDS activity was determined by incubation at 10, 20, 30, 37, 45, and 50 °C, after which, the enzymatic activity was measured. A gradual increase in the enzymatic activity was noticed to correlate with the reaction temperature. The maximum TDS activity by both of the bacterial isolates was recorded at ~40 °C, with a significant reduction to their activity at 50 °C (Figure 5). The upper panel of Figure 6 shows how the released taxadiene byproducts appeared on the plates. The enzymes from both bacterial isolates produced the same reactivity pattern to the reaction temperature. At the 40 °C reaction temperature, the TDS activity from B. koreensis and S. maltophilia were 8.1 µmol/mg/min and 2.5 µmol/mg/min, respectively.
The effect of the reaction mixture pH on the activities of the purified TDS from the experimented bacterial isolates was assessed in the pH range of 4–10 using different buffers. The maximum TDS activity for TDS from B. koreensis and S. maltophilia was reported at pH 7.4. A dramatic decrease in the enzymatic activity of about 75% was measured in acidic conditions (pH 4.0), this was in contrast to the enzymatic activity being quite stable at slightly alkaline pHs (pH 10.0).
The effect of the thermal stability of purified TDS from both bacterial isolates was assessed by preincubating the enzyme without substrate and then measuring the residual enzymatic activity using the standard assay. From the thermal stability profile, the catalytic structure of the purified enzyme was dramatically reduced with the preincubation of the enzyme at a higher temperature (Figure 5), as revealed from the thermal stability parameters (Table 4). At 4 °C, the half-life time (T1/2) of the TDS from B. koreensis and S. maltophilia was 136.0 h and 98 h, respectively, while at 37 °C, the half-life time (T1/2) was 46.0 h and 48.0 h for the purified TDS from B. koreensis and S. maltophilia, respectively. The half-life temperature (Tm) for the TDS from B. koreensis and S. maltophilia was 61.3 and 49.7 °C, respectively. The purified TDS from B. koreensis displayed relatively better thermal and catalytic stability than S. maltophilia, as revealed from the thermal inactivation rate at 37 °C, showing values of 0.15 × 10−3 and 0.24 × 10−3, respectively. The taxadiene that was released TDS as a byproduct and that consumed GGPP is shown as it appeared on the TLC plate in the upper panel of Figure 5. Thus, from the thermal stability kinetics and the molecular subunit structure, the purified TDS from both bacterial isolates displayed slightly structural/conformational differences.

3.6. Effect of Inhibitors and Amino Acid Suicide Analogues on the Activity of TDS

The active sites and structural identities of the purified TDS from both bacterial isolates in response to various inhibitors and amino acid suicide analogues were estimated. The purified enzyme preparations were demetallized, and then the apoenzyme were amended with different inhibitors for 2 h at 4 °C, and the residual activity was measured by the standard assay. From the results (Figure 6), the purified Apo-TDS from both bacterial isolates lost about 50% of their initial activity upon demetallization, ensuring the metalloproteinic identity of this enzyme. The activity of the purified TDS was restored completely upon the addition of Mg2+, confirming the identity of this enzyme on Mg2+ as a cofactor. However, the activity of the purified enzyme was slightly inhibited upon the addition of other metals cations compared to Apo-TDS enzyme preparation. These results reveal the dependence of purified TDS on the Mg2+ essential cofactor. The taxadiene that was released as an enzymatic byproduct from the purified TDS is shown as it appeared on the TLC plate (upper panel, Figure 6). The active sites and allosteric sites of the purified TDS were mapped using different amino acid analogues [40,41,42,47,50,51,52]. The activity of the purified TDS from both bacterial isolates was dramatically reduced by about 60 and 50% upon the addition of DTNB and MBTH, respectively (Figure 6), ensuring the implementation of reactive thiols and ammonia groups on the active site domains of the purified TDS. The TDS activity from both bacterial sources was slightly reduced by about 20–25% in response to hydroxylamine, iodoacetate, and guanidine thiocyanate compared to the control enzymes.

4. Discussion

Taxadiene synthase is the committed rate-limiting enzyme of Taxol biosynthesis by the cyclization of GGPP into taxadiene that has been previously characterized in Taxus brevifolia [2,4]. Taxol-producing potency from endophytic fungi has been frequently reported [5,6,9,10,16,18,19]; however, the attenuation/loss of the fungal biosynthetic potency of Taxol is the major challenge that is preventing the ongoing industrial implementation of this approach. Several hypotheses have been proposed to unravel the physiological and metabolic vagueness of the attenuation of the fungal biosynthetic potency of Taxol, as extensively reported by several studies [11,13,53,54]. Among these metabolic traits, the dependence of the biosynthetic machinery of Taxol by fungi on the external signals from the surrounding microbiome is the most authenticated factor [9,19,55,56]. Triggering the expression and functionality of TDS as the rate limiting enzyme of Taxol biosynthesis is one the most noticeable metabolic criterion in response to the cocultivation with different Taxol-eliciting bacteria [55,57]. Thus, the characterization and subsequent overexpression of this enzyme on Taxol-producing fungal isolates could emphasize and stabilize the biosynthetic potency of Taxol by potent fungal isolates. As such, this study provides motivation for the further exploration of the taxadiene synthase/diterpene cyclase with robust catalytic efficiency and turnover number from different bacterial isolates.
Twenty-three endophytic bacterial isolates were recovered from the leaves of M. piperita L., Coriandrum sativum L., A. graveolens L., M. oleifera Lam., and P. gracilior. Among the recovered bacteria, the highest TDS productivity were determined with B. koreensis and S. maltophilia, which were been identified based on their 16S rDNA sequence and deposited on genbank with the accession # MN592666.1 and MN592660, respectively. The chemical identity of the released putative taxadiene as an enzymatic byproduct of purified TDS” was confirmed in the GC-MS analysis, as it produced the same fragmentation pattern as the parent and daughter molecules of authentic taxadiene. Although, the catalytic identity of the purified terpene cyclase is the same as the taxadiene synthase from the target bacterial isolates, these bacterial isolates lack the ability to naturally produce taxadiene and Taxol. The molecular mass of the taxadiene parent molecule is 271.2 m/z compared to that of authentic taxadiene, which is 272.1 m/z [3,27]. Interestingly, this is the first report exploring taxadiene production from these bacterial isolates. However, different types of terpenoids have frequently been reported to be produced from certain filamentous bacteria [58], such as from Cyanobacteria [59] and Myxobacteria [60] and fungal isolates [5,9,46]. Among the different types of bacteria, filamentous ones “Actinomycetes” are the superior terpenoids for the production of prokaryotes, as extensively reviewed [20,23,60,61]. Unlike the uncountable number of terpenoids from bacteria [20], this is the first study exploring Taxadiene biosynthesis from bacteria. Nevertheless, the metabolic engineering of B. subtilis for taxadiene synthesis, “the first committed step in Taxol production”, was conducted by expressing the plant-derived taxadiene synthase and other enzymes that are able to increase the flux of GGPP precursors [27]. Intriguingly, this is the first study to explore the natural production of taxadiene from B. koreensis and S. maltophilia, which could provide a novel strategy for commercial Taxol production [6,9,19].
To validate TDS activity and taxadiene productivity, the tds gene was amplified by PCR with the nested primers that were designed based on the conserved active-site sequences of TDS from different fungal and plant sources (Taxus brevifolia and T. baccata) [6,9,19]. The active sites of the tds genes exhibited a highly conserved aspartate-rich motif DDXX(X)(D,E) and an NSE triad ND(L,I,V)XSXXXE that were involved in Mg2+ cofactor binding [62]. The amplicons of tds1 and tds2 from both bacterial isolates B. koreensis and S. maltophilia were sequenced and analyzed using the BLAST alignment tool from NCBI. From the alignment profile, the partial sequence of the putative tds of B. koreensis displayed 90–99% similarity with the tds of T. brevifolia and T. baccata and A. flavipes [61]. The PCR screening of the tds and dbat signature genes, “rate-limiting enzymes of Taxol biosynthesis”, were independently authenticated i for different microbes [63,64,65,66].
The productivity of the taxadiene synthase by B. koreensis and S. maltophilia was nutritionally optimized with the surface response methodology using nineteen independent variables. Upon using the Plackett–Burman design, the TDS activity increased from 2.2 to 18.0 µmol/mg/min, reflecting the significance of the independent variables. The maximum TDS activity achieved by B. koreensis was obtained in presence sucrose (1 g), peptone (5 g), ammonium nitrate (4 g), tryptophan (1 g), tyrosine (1 g), glucose (1 g), glutamic acid (1 g), glycine (1 g), and methionine (4 g) per liter of distilled water, at pH 6.0, and after 6 days of incubation. The correlation of TDS productivity with the independent variables was assessed by the multiple-regression statistical analysis of variance (ANOVA) of the experimental design, as revealed from the p-value and student’s t-test. Thus, upon using the Plackett–Burman design, the TDS productivity achieved by B. koreensis increased by about 2.1-fold. Similar results were reported when optimizing the productivity of the microbial enzymes upon nutritional optimization [35,39].
The enzymes were purified using the gel-filtration and ion-exchange chromatographic approaches to determine its molecular homogeneity, which was confirmed by SDS-PAGE. The purified TDS from both of the bacterial isolates displayed a relative proximity on their molecular mass and overall charge. The activity of the TDS from B. koreensis and S. maltophilia increased by about 15.9- and 14.6- folds, respectively, upon the use of this purification protocol. The entire molecular mass of the purified TDSs from both of the bacterial isolates was approximately 180 kDa on native-PAGE, while the TDS subunit structure from B. koreensis and S. maltophilia were 65 and 80 kDa, respectively, under denaturing-PAGE [3,31]. The purified TDS from the bacterial isolates had two identical subunits with a homodimeric identity, which was consistent with the overexpressed TDS achieved by the T. baccata in B. subtilis [24,27].
The biochemical and kinetic properties of the purified TDSs were determined. The maximum activity of the TDS from both bacterial isolates was recorded at 37–40 °C. At 4 °C, the half-life time (T1/2) of TDS from B. koreensis and S. maltophilia was 136.0 h and 98 h, respectively. The half-life temperature (Tm) for the purified TDS from B. koreensis and S. maltophilia was 61.3 and 49.7 °C, respectively, ensuring the slight thermal stability of TDS produced from B. koreensis than S. maltophilia. This is partially consistent with the highest activity achieved by T. baccata, where TDS was reported at 20 °C, with no activity at 37 °C [27], revealing the significant thermal stability of purified the TDS produced by B. koreensis and S. maltophilia. This obvious catalytic efficiency and stability could be related to the amino acid sequence domains and tertiary structure of the TDS produced from these bacterial isolates during posttranslational modification since the TDS from T. baccata is naturally expressed as a pseudo-mature enzyme of 862 amino acids with splicing of 60 amino acids as a plastidal signal sequence during the maturation process [67]. Thus, the thermal stability of TDS produced from B. koreensis and S. maltophilia is better than TDS produced from different plant sources, making it a feasible/unique biochemical criterion. Further molecular modelling and crystal structure studies aiming to resolve the molecular structure of the current TDS compared to TDS from T. baccata are ongoing.
The maximum TDS activity for TDS from B. koreensis and S. maltophilia was reported at pH 7.4–8.0. A dramatic decrease to the enzymatic activity by about 75% was measured at acidic conditions (pH 4.0), which is unlike the quite good enzymatic activity stability seen at slightly alkaline pHs (pH 10.0). Similar results were reported for TDS from T. baccata [68] and T. canadensis [69].
The active sites and structural identities of purified TDS from both bacterial isolates in response to various inhibitors and amino acid suicide analogues were mapped. Apo-TDSs retained ~50% of the initial activities of holo-TDS, ensuring the metalloproteinic identity of this enzyme. The activity of purified TDS was completely restored upon the addition of Mg2+, confirming the identity of this enzyme on Mg2+ as a cofactor [57,68]. However, the activity of the purified enzyme was slightly inhibited upon the addition of other metals cations compared to Apo-TDS enzyme preparation. The purified TDS activity was dramatically reduced by upon the addition of DTNB and MBTH, respectively, ensuring the implementation of reactive thiols and ammonia groups on their active site domains [41,42,43,45,49,50,52,70,71]. Similar studies ensure the metalloproteinic identity of TDS from T. brevifolia and T. baccata [3,57,69].
In conclusion, taxadiene synthase was purified from B. koreensis and S. maltophilia, which had higher catalytic efficiency to cyclize GGPP into taxadiene as the rate limiting step in Taxol biosynthesis. The chemical identity of taxadiene was authenticated from the GC-MS analysis by comparing it to the authentic one. In addition to the colorimetric activities of TDS, the active site domains of tds were amplified by PCR, which were sequenced and displayed more similarity to those from T. baccata and T. brevifolia. Although the subunit structure and metalloproteinic of TDS of B. koreensis and S. maltophilia was similar to that of the T. baccata TDS, the purified enzyme displayed plausibly higher thermal stability and catalytic efficiency. This is the first report describing TDS from bacteria with a higher affinity to cyclize GGPP into taxadiene as a rate-limiting step in Taxol biosynthesis; thus, furthering the overexpression analysis of TDS on fungi could be a new strategy for sustaining the biosynthetic machinery of Taxol in the target fungi.

Supplementary Materials

The following are available online at https://www.mdpi.com/article/10.3390/scipharm89040048/s1.

Author Contributions

A.S.A.E.-S. conceptualized the work; M.F. and M.S. designed the work; A.S.A.E.-S. wrote the manuscript; A.M.R. conducted the statistical analysis; A.F.E.-B. completed the factorial design optimization analysis; A.F.E.-B. and A.A.S. revised the manuscript; Y.M. performed the experimental work; B.S. edited the manuscript. All authors have read and agreed to the published version of the manuscript.

Funding

We appreciate the financial support from the Academy of Scientific Research and Technology, Egypt, to Ashraf S.A. El-Sayed and the support from the Medical Faculty of Umea University, the Council of Vasterbotten, and Lions Cancer Research Fund to Basel Sitohy.

Institutional Review Board Statement

Not applicable.

Data Availability Statement

All data generated during this study are included in the article.

Acknowledgments

We appreciate the financial support from the Egyptian Academy of Scientific Research and Technology (ASRT) to A.S.A.E. All the authors have consented to the acknowledgment.

Conflicts of Interest

The authors declare that they have no conflict interests.

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Scipharm 89 00048 g001 550
Figure 1. Screening for TDS production from different bacteria isolates. After incubation, the bacterial cultures were pelleted, the intracellular proteins were isolated, and the activity of crude TDS was determined. The TLC chromatogram of the residual GGPP (A) and the putative TDS activity (B) is shown. PCR amplification of tds from the selected bacterial producers using the active-site conservative primers TDS1 (C) and TDS2 (D) is shown.
Figure 1. Screening for TDS production from different bacteria isolates. After incubation, the bacterial cultures were pelleted, the intracellular proteins were isolated, and the activity of crude TDS was determined. The TLC chromatogram of the residual GGPP (A) and the putative TDS activity (B) is shown. PCR amplification of tds from the selected bacterial producers using the active-site conservative primers TDS1 (C) and TDS2 (D) is shown.
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Figure 2. GC-MS analysis of the released taxadiene as a byproduct of putative crude TDS from Bacillus koreensis. After incubation of the enzymatic reaction, the enzymatic byproducts were spotted on TLC, and putative taxadiene spots were scraped-off of the silica gel particles and were analyzed by GC-MS analysis. (A) TLC chromatogram of enzymatic byproduct. (B) Spectrum of counts vs. acquisition time. (C) Mass spectrum of putative taxa-4,11-diene with the inset chemical formula.
Figure 2. GC-MS analysis of the released taxadiene as a byproduct of putative crude TDS from Bacillus koreensis. After incubation of the enzymatic reaction, the enzymatic byproducts were spotted on TLC, and putative taxadiene spots were scraped-off of the silica gel particles and were analyzed by GC-MS analysis. (A) TLC chromatogram of enzymatic byproduct. (B) Spectrum of counts vs. acquisition time. (C) Mass spectrum of putative taxa-4,11-diene with the inset chemical formula.
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Figure 3. Molecular identification of potent TDS-producing bacterial isolates. PCR amplicons of the selected bacterial isolates using their genomic DNA as a template for PCR with the primers for 16S rDNA (A). Molecular phylogenetic analyses of Stenotrophomonas maltophilia (B) and Bacillus koreensis (C) by the maximum likelihood model in the MEGA 7.0 package.
Figure 3. Molecular identification of potent TDS-producing bacterial isolates. PCR amplicons of the selected bacterial isolates using their genomic DNA as a template for PCR with the primers for 16S rDNA (A). Molecular phylogenetic analyses of Stenotrophomonas maltophilia (B) and Bacillus koreensis (C) by the maximum likelihood model in the MEGA 7.0 package.
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Figure 4. Purification and molecular subunit structure of TDS from S. maltophilia and B. koreensis. The bacterial pellets were pulverized in liquid nitrogen and were dispensed in Tris-HCl buffer with protease inhibitors, as described in the Materials and Methods sections. TDS activity resulting from the ion-exchange (A) and gel-filtration (B) chromatographic approaches for both bacterial isolates. The SDS-PAGE profile showing the molecular subunit structure of purified TDS (C) and native-PAGE displaying the entire molecular mass of TDS (D) from both bacterial isolates. The numbers 1 and 2 on the gels refer to Bacillus koreensis and S. maltophilia, respectively. M is the protein ladder (Blue Plus Protein Maker, Cat. # DM101, 14–100 kDa).
Figure 4. Purification and molecular subunit structure of TDS from S. maltophilia and B. koreensis. The bacterial pellets were pulverized in liquid nitrogen and were dispensed in Tris-HCl buffer with protease inhibitors, as described in the Materials and Methods sections. TDS activity resulting from the ion-exchange (A) and gel-filtration (B) chromatographic approaches for both bacterial isolates. The SDS-PAGE profile showing the molecular subunit structure of purified TDS (C) and native-PAGE displaying the entire molecular mass of TDS (D) from both bacterial isolates. The numbers 1 and 2 on the gels refer to Bacillus koreensis and S. maltophilia, respectively. M is the protein ladder (Blue Plus Protein Maker, Cat. # DM101, 14–100 kDa).
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Figure 5. Biochemical properties of TDS from S. maltophilia and B. koreensis. The effect of reaction temperature (A), reaction pH (B), thermal stability profiles of B. koreensis (C), and S. maltophilia (D). For each assay, the TLC chromatogram of the residual GGPP is placed in the upper panel, while the actual activity of TDS is in the lower panel. (E), Profile of half-life temperature (Tm) of purified TDS of S. maltophilia and B. koreensis.
Figure 5. Biochemical properties of TDS from S. maltophilia and B. koreensis. The effect of reaction temperature (A), reaction pH (B), thermal stability profiles of B. koreensis (C), and S. maltophilia (D). For each assay, the TLC chromatogram of the residual GGPP is placed in the upper panel, while the actual activity of TDS is in the lower panel. (E), Profile of half-life temperature (Tm) of purified TDS of S. maltophilia and B. koreensis.
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Figure 6. Effect of cation inhibitors and amino acid suicide analogues on the purified TDS from S. maltophilia and B. koreensis. The purified TDS from both bacterial isolates were dialyzed with EDTA, apo-enzyme was concentrated and amended with different inhibitors, and the residual activity of the enzymes was determined by the standard assay as described in the Materials and Methods section. The TLC chromatogram of the TDS reaction mixture is in the upper panel, and the actual activity is in the lower panel. The TDS activity in response to cation inhibitors (A) and various active-site amino acid suicide analogues (B).
Figure 6. Effect of cation inhibitors and amino acid suicide analogues on the purified TDS from S. maltophilia and B. koreensis. The purified TDS from both bacterial isolates were dialyzed with EDTA, apo-enzyme was concentrated and amended with different inhibitors, and the residual activity of the enzymes was determined by the standard assay as described in the Materials and Methods section. The TLC chromatogram of the TDS reaction mixture is in the upper panel, and the actual activity is in the lower panel. The TDS activity in response to cation inhibitors (A) and various active-site amino acid suicide analogues (B).
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Table
Table 1. Experimental independent variables at two levels used for TDS production by the Plackett–Burman design.
Table 1. Experimental independent variables at two levels used for TDS production by the Plackett–Burman design.
CodeVariablesLevel
−11
X1Yeast extract (g/L)14
X2Peptone (g/L)15
X3Phenylalanine (g/L)14
X4Tyrosine (g/L)14
X5Tryptophan (g/L)14
X6Glycine (g/L)14
X7Valine (g/L)14
X8Methionine (g/L)14
X9Asparagine (g/L)14
X10Cysteine (g/L)14
X11Glutamic acid (g/L)14
X12Beef extract (g/L)14
X13Sucrose (g/L)15
X14Glucose (g/L)15
X15Xylose, (g/L)15
X16NaCl (g/L)26
X17Ammonium nitrate (g/L)14
X18pH68
X19Incubation period (day)36
Table
Table 2. The twenty-trial Plackett–Burman experimental design for evaluation of the independent variables with coded values along with the observed TDS production by B. koreensis. The “−1′′ sign corresponds to the minimum value, and the “+1′′ sign corresponds to the maximum value of the input parameter range.
Table 2. The twenty-trial Plackett–Burman experimental design for evaluation of the independent variables with coded values along with the observed TDS production by B. koreensis. The “−1′′ sign corresponds to the minimum value, and the “+1′′ sign corresponds to the maximum value of the input parameter range.
g/L 12345678910111213141516171819
Run X1X2X3X4X5X6X7X8X9X10X11X12X13X14X15x16X17X18X19Predicted TDS Activity
1−1−1−1−111−111−1−11111−11−112.263.465
2111−11−11−1−1−1−111−111−1−111.82.85
311−111−1−11111−11−11−1−1−1−12.273.55
41−11−11−1−1−1−111−111−1−11113.785.85
5−1−111−111−1−11111−11−11−1−10.81.25
6−1−1−1−1−1−1−1−1−1−1−1−1−1−1−1−1−1−1−16.9810.92
7−111−1−11111−11−11−1−1−1−1116.7810.52
81111−11−11−1−1−1−111−111−1−16.099.55
9−11111−11−11−1−1−1−111−111−17.0810.95
10−1−11111−11−11−1−1−1−111−1115.608.765
111−111−1−11111−11−11−1−1−1−115.037.86
121−1−1−1−111−111−1−11111−11−15.678.85
13−111−111−1−11111−11−11−1−1−12.583.95
141−11−1−1−1−111−111−1−11111−111.7218.3
15−1−1−111−111−1−11111−11−11−12.123.3
16−1−1−11111−11−11−1−1−1111−111.181.75
1711−11−11−1−1−1−111−111−1−1114.076.35
18−11−1−1−1−111−111−1−11111−115.568.68
19−11−11−1−1−1−111−111−1−111116.5610.25
2011−1−11111−11−11−1−1−1−111−110.4616.35
Table
Table 3. Purification profile of TDS from B. koreensis and S. maltophilia.
Table 3. Purification profile of TDS from B. koreensis and S. maltophilia.
StepB. koreensisS. maltophilia
Total Protein (mg) Total Activity (µmol/min)Specific Activity (µmol/mg/min) Yield (%) Purification Fold Total Protein (mg) Total Activity (µmol/min)Specific Activity (µmol/mg/min) Yield (%) Purification Fold
Crude enzyme413.6177.60.43100165078.20.131001
Acetone precipitate87.560.90.734.31.658639.50.5452.64.48
Sephadex-G20032.340.61.2622.92.923.930.51.2950.010.6
DEAE-Sepharose0.53.426.8419.215.95.69.81.716.914.6
Table
Table 4. Thermal kinetic parameters of TDS from B. koreensis and S. maltophilia.
Table 4. Thermal kinetic parameters of TDS from B. koreensis and S. maltophilia.
°CB. koreensisS. maltophilia
T1/2 (h) *Kr (min) **Tm (°C) ***T1/2 (h) *Kr (min) **Tm (°C) ***
4136.00.02 × 10−361.3980.03 × 10−349.7
2066.40.1 × 10−3680.14 × 10−3
37460.15 × 10−3480.24 × 10−3
45230.24 × 10 −3240.30 × 10−3
50100.29 × 10−3110.32 × 10−3
* Half-life time (T1/2) was expressed by the time in which the enzyme retained 50% of its initial activity by preheating it without substrate at each temperature degree. ** ln (At/A0) = −Kr Tm, where A0 and At are the specific TDS activity at zero and t time. *** Thermal denaturation rate (Kr) was expressed by the logarithmic decreasing of enzyme activity with the time at each temperature, as defined from the first-order kinetic model.
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El-Sayed, A.S.A.; Fathalla, M.; Shindia, A.A.; Rady, A.M.; El-Baz, A.F.; Morsy, Y.; Sitohy, B.; Sitohy, M. Purification and Biochemical Characterization of Taxadiene Synthase from Bacillus koreensis and Stenotrophomonas maltophilia. Sci. Pharm. 2021, 89, 48. https://doi.org/10.3390/scipharm89040048

AMA Style

El-Sayed ASA, Fathalla M, Shindia AA, Rady AM, El-Baz AF, Morsy Y, Sitohy B, Sitohy M. Purification and Biochemical Characterization of Taxadiene Synthase from Bacillus koreensis and Stenotrophomonas maltophilia. Scientia Pharmaceutica. 2021; 89(4):48. https://doi.org/10.3390/scipharm89040048

Chicago/Turabian Style

El-Sayed, Ashraf S. A., Maher Fathalla, Ahmed A. Shindia, Amgad M. Rady, Ashraf F. El-Baz, Yara Morsy, Basel Sitohy, and Mahmoud Sitohy. 2021. "Purification and Biochemical Characterization of Taxadiene Synthase from Bacillus koreensis and Stenotrophomonas maltophilia" Scientia Pharmaceutica 89, no. 4: 48. https://doi.org/10.3390/scipharm89040048

APA Style

El-Sayed, A. S. A., Fathalla, M., Shindia, A. A., Rady, A. M., El-Baz, A. F., Morsy, Y., Sitohy, B., & Sitohy, M. (2021). Purification and Biochemical Characterization of Taxadiene Synthase from Bacillus koreensis and Stenotrophomonas maltophilia. Scientia Pharmaceutica, 89(4), 48. https://doi.org/10.3390/scipharm89040048

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