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Green route to synthesis of valuable chemical 6-hydroxynicotine from nicotine in tobacco wastes using genetically engineered Agrobacterium tumefaciens S33
Biotechnology for Biofuelsvolume 10, Article number: 288 (2017)
Tobacco is widely planted as an important nonfood economic crop throughout the world, and large amounts of tobacco wastes are generated during the tobacco manufacturing process. Tobacco and its wastes contain high nicotine content. This issue has become a major concern for health and environments due to its toxicity and complex physiological effects. The microbial transformation of nicotine into valuable functionalized pyridine compounds is a promising way to utilize tobacco and its wastes as a potential biomass resource. Agrobacterium tumefaciens S33 is able to degrade nicotine via a novel hybrid of the pyridine and pyrrolidine pathways, in which several intermediates, such as 6-hydroxynicotine, can be used as renewable precursors to synthesize drugs and insecticides. This provides an opportunity to produce valuable chemical 6-hydroxynicotine from nicotine via biocatalysis using strain S33.
To accumulate the intermediate 6-hydroxynicotine, we firstly identified the key enzyme decomposing 6-hydroxynicotine, named 6-hydroxynicotine oxidase, and then disrupted its encoding gene in A. tumefaciens S33. With the whole cells of the mutant as a biocatalyst, we tested the possibility to produce 6-hydroxynicotine from the nicotine of tobacco and its wastes and optimized the reaction conditions. At 30 °C and pH 7.0, nicotine could be efficiently transformed into 6-hydroxynicotine by the whole cells cultivated with glucose/ammonium/6-hydroxy-3-succinoylpyridine medium. The molar conversion and the specific catalytic rate reached approximately 98% and 1.01 g 6-hydroxynicotine h−1 g−1 dry cells, respectively. The product could be purified easily by dichloromethane extraction with a recovery of 76.8%, and was further confirmed by UV spectroscopy, mass spectroscopy, and NMR analysis.
We successfully developed a novel biocatalytic route to 6-hydroxynicotine from nicotine by blocking the nicotine catabolic pathway via gene disruption, which provides an alternative green strategy to utilize tobacco and its wastes as a biomass resource by converting nicotine into valuable hydroxylated-pyridine compounds.
Tobacco is widely planted as an important nonfood economic crop throughout the world, and large amounts of tobacco wastes are generated during the tobacco manufacturing process [1,2,3]. Nicotine, the main toxic alkaloid in tobacco leaves and its wastes, comprises approximately 0.6–5% (w/w) of tobacco dry materials and is responsible for tobacco addiction and environmental threats [1, 4]. Nicotine was listed in the Toxics Release Inventory by the US Environmental Protection Agency as early as 1994. It has complex physiological effects and may cause diseases such as cancer [5,6,7]. Thus, the treatment of nicotine becomes the major concern for tobacco waste disposal. In 2003, the WHO framework convention on tobacco control led to great negative effects regarding the cultivation of tobacco. Therefore, it is imperative to develop efficient technologies to deal with tobacco wastes and utilize tobacco leaves. Nowadays, wastes are often considered as potential resources. Replacing waste disposal with resource recovery is a green method for saving energy . Microbiologists have been engaged in research regarding various applications of tobacco and its wastes because of their high nicotine content, for example, the biotransformation of nicotine into its valuable intermediates, the functionalized pyridines, using nicotine-degrading microorganisms [9,10,11,12,13,14]. Agrobacterium tumefaciens S33, previously isolated from the tobacco rhizosphere, has a strong ability to degrade nicotine via a hybrid of the pyridine and pyrrolidine pathways (Fig. 1a) [4, 11]. It is interesting that at least three intermediates (6-hydroxynicotine, 6-hydroxy-3-succinoylpyridine [HSP], and 2,5-dihydroxypyridine) in this pathway can be used as renewable precursors to synthesize drugs and insecticides via chemical methods. This is due to the hydroxylation of pyridines at the 6-position or 2- and 5-positions, which can be modified easily via specific and efficient biocatalytic processes . 6-Hydroxynicotine and HSP can be used as valuable precursors to synthesize biologically active 2,5- or 3,5-substituted pyridines, such as the insecticide imidacloprid, the anti-Parkinson’s agent SIB-1508Y, and analogs of the potent analgesic Epibatidine, which has obvious paregoric effects [9, 10, 15]. Furthermore, 6-hydroxynicotine and some derivatives perform functions for memory enhancement and oxidation resistance , transgene expression induction , and microbial resistance [18, 19]. Consequently, using nicotine to produce valuable compounds through a combination of biocatalysis and chemocatalysis offers the possibility for developing new applications for tobacco and its wastes.
Biocatalysis with microbial whole cells is a promising process for industrial production [10, 20]. Compared with chemical methods, biocatalysis is safer, more specific, more sustainable, and more environmentally friendly. The reaction conditions are also less stringent. Compared with the use of enzymes as biocatalysts, whole cells can be repetitively and economically utilized, and their cofactor regeneration is much easier and less expensive . As a result, biocatalysis based on whole cells provides a continuous process for environmentally friendly energy recovery. However, throughout the whole-cell reaction process, the valuable intermediates of nicotine degradation continue to be further catabolized by the wild-type strains cells [9, 12, 19], leading to a low molar conversion and the formation of by-products that cause difficulties for product purification. For this reason, greater efforts are required for the optimization of biocatalyst preparation and catalytic conditions. Recently, great interest has been aroused regarding the development of novel biocatalytic processes to achieve high efficiency and selectivity. Thus, engineered bacteria have been suggested as a potential solution, presenting a new approach for the use and control of microbial transformations [21, 22]. By deleting one or several genes required for catabolism, the nicotine degradation pathway is blocked, and the accumulation of valuable intermediates is achieved [13, 14].
Herein, the efforts were put forth to test the transformation of nicotine into 6-hydroxynicotine by A. tumefaciens S33, knowing that this strain harbors nicotine dehydrogenase (NdhAB) that can catalyze nicotine hydroxylation at the 6-position of the pyridine ring with pseudoazurin as its electron acceptor (Fig. 1a) [23, 24]. First, we purified and characterized the key enzyme 6-hydroxynicotine oxidase (Hno) that catalyze the oxidation of 6-hydroxynicotine to 6-hydroxy-N-methylmyosmine in A. tumefaciens S33. Then, the hno gene of strain S33 was disrupted, causing the degradation of nicotine to be blocked at 6-hydroxynicotine (Fig. 1b). After optimizing the reaction conditions and the biocatalyst preparation conditions, we developed a novel and efficient green route for producing 6-hydroxynicotine with the whole cells of the engineered hno-disrupted strain S33 as the catalyst.
Results and discussion
Purification of Hno from A. tumefaciens S33 and identification of its encoding gene
In our previous study on purification of NdhAB, three yellow-colored fractions adjacent to the NdhAB-containing fractions were found to have 6-hydroxynicotine oxidation activity after separation by DEAE Fast Flow column . The protein was further purified by applying to Q Sepharose and eluted with 0.25 M NaCl, which was nearly pure, as detected by SDS-PAGE (Fig. 2a), and presented a specific 6-hydroxynicotine oxidation activity of 12.0 ± 1.4 μmol min−1 mg−1. To identify its encoding genes, the purified protein was analyzed using MALDI-TOF/MS. The MS results were searched against the annotated genome of A. tumefaciens S33 [25, 26]. We found that the enzyme was encoded by an ORF of 1314 bp, designated as hno, which formed one large gene cluster together with the genes for NdhAB, Pno, and Hsh (Fig. 1b); however, its transcription direction was opposite to ndhAB. The identification of the hno gene was supported also by our previous transcriptomic analysis, where a log2 ratio (FPKM of Nic/FPKM of Glu) (FPKM, fragments per kilobase per million) of 5.9 for the hno gene was observed in nicotine medium (Nic) and glucose–ammonium medium (Glu) . The deduced protein sequence (437 amino acids, 48.76 kDa) has 99.8% identity to both 6-hydroxynicotine oxidase NctB from Shinella sp. HZN7  and 6-hydroxynicotine oxidase VppB from Ochrobactrum sp. SJY1 , 38.9% to nicotine oxidase Nox from Pseudomonas sp. HZN6 , 38.4% to nicotine oxidoreductase NicA2 from P. putida S16 , and 24.8% to 6-hydroxy-l-nicotine oxidase from A. nicotinovorans [31, 32]. All these proteins harbor a conserved FAD-binding motif, suggesting that Hno in strain S33 is also a flavin-containing oxidoreductase.
Heterologous production and properties of recombinant Hno
In order to confirm the function of the hno gene, we heterologously expressed it in E. coli BL21 (DE3) with a His tag at the N-terminus and purified the recombinant protein using His Trap HP and DEAE Sepharose Fast Flow columns (Fig. 2b). A single band with an apparent molecular mass of 50 kDa was detected by SDS-PAGE, which was identical to the calculated molecular mass of the His-tagged Hno and wild-type Hno purified from A. tumefaciens S33 (Fig. 2a). HPLC analysis showed that the yellow protein contained a FAD, which was consistent with the fact that the protein harbors a Rossmann-like domain, as shown by conserved domain analysis in NCBI, and exhibited a typical absorption of flavin at 382 and 459 nm (Fig. 2c). Enzyme assays showed that at 37 °C and pH 9.2 (100 mM Glycine–NaOH buffer), the enzyme showed a V max of 26.43 ± 0.16 U/mg, and an apparent K m for 6-hydroxynicotine of 0.067 ± 0.001 mM (Fig. 2d), which are both similar to the kinetic constants of NctB and VppB from Shinella sp. HZN7  and Ochrobactrum sp. SJY1 , respectively.
The reaction products catalyzed by the purified Hno were analyzed by UV–visible spectrophotometer. The absorption spectra (Fig. 2e) showed that the absorption of the substrate 6-hydroxynicotine (maximum absorption at 295 nm) decreased and a new peak appeared (maximum absorption at 334 nm), indicating that 6-hydroxynicotine was transformed into other compounds. The products were further analyzed by LC–MS (Fig. 3). Three large peaks were found in the chromatography (retention time as 4.90, 5.31, and 6.67 min, respectively) (Fig. 3), and monitored with a photodiode array (PDA) detector. The mass-to-charge ratios (m/z) of the main fragments in the mass spectra are identical to the calculated molecular mass of 6-hydroxynicotine (peak a, m/z 179.1), 6-hydroxy-N-methylmyosmine (peak b, m/z 177.1), and 6-hydroxypseudooxynicotine (peak c, m/z 195.1). This indicates that Hno transforms 6-hydroxynicotine into the 6-hydroxy-N-methylmyosmine, which then is converted spontaneously into 6-hydroxypseudooxynicotine, just like the reaction catalyzed by 6-hydroxy-l-nicotine oxidase in the pyridine pathway of A. nicotinovorans . These results confirm that Hno from strain S33 is a FAD-containing oxidase and that it catalyzes the second step of 6-hydroxynicotine oxidation in the hybrid nicotine degradation pathway.
Construction of the strain with disrupted hno gene and its complementation strain
To block the 6-hydroxynicotine oxidization by Hno in the nicotine-degrading pathway of strain S33, we disrupted the hno gene with the plasmid pJQ200SK harboring the truncated target gene and then complemented with the plasmid pBBR1MCS-5 containing a complete copy of hno. Growth tests showed that the mutant strain S33-∆hno could grow well in lysogeny broth (LB) (Fig. 4a) and HSP media (Fig. 4b) but not in nicotine (Fig. 4c) or 6-hydroxynicotine media (Fig. 4d), while the wild-type strain and the complemented strain S33-∆hno-C could grow in all media. The results confirm that the hno gene is responsible for the oxidation of 6-hydroxynicotine and is required for nicotine degradation in strain S33. The mutant strain S33-∆hno lost the ability to further catabolize 6-hydroxynicotine.
The activities of NdhAB and Hno in all strains were measured when they were grown in HSP medium or nicotine–glucose–ammonium medium (Table 1). The results showed that Hno activity was not detected in the mutant strain S33-∆hno. Interestingly, when strain S33-∆hno was cultured in HSP medium, its Ndh activity was much higher than when cultured in nicotine–glucose–ammonium medium.
Testing the biotransformation of nicotine into 6-hydroxynicotine catalyzed by whole cells of A. tumefaciens S33-∆hno
To determine the possibility of 6-hydroxynicotine production from nicotine, the biotransformation reaction was performed using whole cells of A. tumefaciens S33-∆hno (~ 1.45 g L−1, dry cell weight, DCW; ~ 3.6 OD620 nm; one OD unit = 0.41 g L−1 DCW) as a catalyst and 0.85 g L−1 nicotine as the substrate in 50 mM sodium phosphate buffer (pH 7.0). The cells were cultured with nicotine–glucose–ammonium medium in consideration of the high cost of HSP, where nicotine could induce the expression of the ndhAB gene according to the results in Table 1 and previous investigations [24, 25]. The mixture was shaken at 30 °C with a speed of 200 rev min−1 (rpm). Samples were withdrawn and analyzed by HPLC to monitor the consumption of the substrate and the formation of the product. Results showed a significant increasing peak with retention time at 5.2 min and a decreasing peak with retention time at 6.0 min (Fig. 5a), which correspond to 6-hydroxynicotine and nicotine, respectively. Finally, nicotine can be converted completely into 6-hydroxynicotine (Fig. 5b). However, the specific catalytic activity of ~ 0.01 g 6-hydroxynicotine h−1 g−1 dry cells was very low, which needs to be improved.
Optimization of the reaction conditions for the biotransformation of nicotine into 6-hydroxynicotine
To improve the catalytic rate, reaction conditions were optimized. As shown in Fig. 6, the catalytic rate was affected by the amount of A. tumefaciens S33-∆hno whole cells added, the initial concentration of nicotine, pH of the buffer, and the incubation temperature. The catalytic rate rose remarkably with the increasing dry weight of the catalyst (Fig. 6a) and the decreasing initial concentration of nicotine (Fig. 6b); however, the specific catalytic rate did not continue to increase when above 2.7 g L−1 of biocatalyst was added (Fig. 6a). The high concentration of nicotine inhibited the catalytic activity. The optimal pH and temperature for the reaction was around 7.0 (Fig. 6c) and 30 °C (Fig. 6d), respectively, which was in consistent with the optimal growth conditions for A. tumefaciens S33 . Figure 6e shows that oxygen was essential for the reaction although the key enzyme catalyzing nicotine hydroxylation is a pseudoazurin-dependent NdhAB . We speculate that oxygen is the final electron acceptor of nicotine oxidative degradation, which accepts the electron from the reduced pseudoazurin via the respiratory chain. Thus, the pseudoazurin can be regenerated in the biotransformation reaction. For the tested system, a low rotation rate supplied enough oxygen to the reaction (Fig. 6e). Finally, the preparation of the whole-cell biocatalyst was examined. Different media were used for culturing A. tumefaciens S33-∆hno (Fig. 6f), where nicotine or HSP was used as an inducer for expressing the nicotine-degrading enzymes, including NdhAB [24, 25]. The results showed that the cells grown in the media containing HSP presented higher catalytic efficiency, which was even better than those grown on nicotine, while LB was the worst medium for preparing the biocatalyst. This agreed with the results from the enzyme assay for the cell extracts of A. tumefaciens S33-∆hno (Table 1), where HSP demonstrated a better induction for NdhAB activity. In consideration of the cost of HSP and biomass obtained, we chose the glucose–ammonium–HSP medium to culture A. tumefaciens S33-∆hno.
Batch and fed-batch biotransformation reactions
Under the optimal conditions (pH 7.0 and 30 °C), we performed the reaction in 200 mL reaction mixture containing 1 g L−1 nicotine and ~ 1.0 g L−1 DCW whole cells of A. tumefaciens S33-∆hno cultured with glucose–ammonium–HSP medium. For batch biotransformations, the catalyst was collected by centrifugation after the first batch reaction and was re-used for three subsequent reactions. As shown in Fig. 7a, the whole-cell biocatalyst could maintain high activity even after being used in four separate reactions. The highest specific catalytic activity reached approximately 1.01 g 6-hydroxynicotine h−1 g−1 dry cells. For each batch, the molar conversion reached ~ 95%. Due to the inhibitory nature of nicotine (Fig. 6a), we also performed a fed-batch biotransformation (Fig. 7b). During the reaction, we supplemented 1 g L−1 of nicotine three times. In total, 4 g L−1 of nicotine could be transformed completely into 4.70 g L−1 of 6-hydroxynicotine (Fig. 7b). The molar conversion reached ~ 98.4%. However, the catalytic rate gradually decreased as time increased in both batch and fed-batch reactions, which may be due to poor stability of the NdhAB activity in the cells, as previously indicated [23, 24]. These results suggest that a combination of fed-batch reactions and recycled biocatalyst reactions would be feasible and ideal for a large scale biotransformation process. Compared with the growing system developed for producing 6-hydroxynicotine from nicotine by wild-type strain Arthrobacter oxydans , the catalytic process developed in this study presented both higher conversion rates and higher yields. Moreover, the whole cells biocatalysts could be recovered easily by centrifugation and repeatedly used several times, which is helpful for reducing costs and for product purification.
Purification and identification of the product 6-hydroxynicotine
The product 6-hydroxynicotine in the reaction mixture was extracted easily by dichloromethane after removing the cells in the reaction mixture by centrifugation and concentrating the supernatant by rotary evaporation under reduced pressure. Finally, 1.20 g of 6-hydroxynicotine was recovered from 600 mL of reaction mixture containing 2.6 g L−1 of 6-hydroxynicotine (76.9% recovery), where a total of approximately 1.43 g of nicotine was added during the reaction (overall yield, 83.9%, w/w). The purified product showed two characteristic maximum absorption peaks, at 232 and 295 nm, in 0.1 M HCl as indicated by UV–visible absorption spectrum (Fig. 8a), which corresponds to a previous report , as well as to authentic 6-hydroxynicotine (Fig. 2e). LC–MS determination showed a peak with m/z as 179.1198 ([M+H]+) that was identical to the calculated molecular mass of 6-hydroxynicotine (C10H14N2O, 178.1106; Fig. 8b, c). The purified product had an 1H-NMR spectrum (CDCl3, 600 MHz) as follows: δ 1.70 (m, 1H); 1.80 (m, 1H); 1.92 (m, 1H); 2.11 (m, 1H); 2.14 (s, 3H); 2.27 (q, J = 9.2 Hz, 1H); 2.85 (t, J = 8.3 Hz, 1H); 3.19 (td, J = 8.6, 1.8 Hz, 1H); 6.60 (d, J = 9.4 Hz, 1H); 7.27 (d, J = 2.4 Hz, 1H); 7.56 (dd, J = 9.4, 2.5 Hz, 1H); a 13C-NMR spectrum (CDCl3, 150 MHz): δ 22.3 (CH2), 33.7 (CH2), 40.0 (CH3), 56.6 (CH2), 67.6 (CH), 120.5 (C), 121.6 (CH), 132.7 (CH), 141.5 (CH), 165.3 (C) (Additional file 1: Figure S1). The NMR data were consistent with those from the authentic commercial standard 6-hydroxynicotine (Additional file 1: Figure S2) and previous study . These results indicate that the purification of the product 6-hydroxynicotine from the reaction mixture can be achieved practically and easily with a satisfactory yield and purity.
The disposal and detoxification of nicotine from tobacco and its wastes are a challenge for the tobacco industry. However, this biomass could be used as a potential resource to recover energy. In this study, we transformed nicotine from tobacco and its wastes into the valuable intermediate 6-hydroxynicotine using a nicotine-degrading A. tumefaciens S33 mutant, in which the enzyme NdhAB catalyzed nicotine hydroxylation with pseudoazurin as its electron acceptor. To accumulate quantities of the intermediate product, we identified the key enzyme Hno, responsible for further oxidative degradation of 6-hydroxynicotine, and disrupted its encoding gene to block the catabolism of 6-hydroxynicotine. With whole cells of the mutant as the biocatalyst, pseudoazurin, the electron acceptor for NdhAB, was regenerated by transferring its electrons to O2 via the respiration chain. At 30 °C and pH 7.0, nicotine was nearly completely transformed into 6-hydroxynicotine by the mutant whole cells; the biocatalyst with the highest nicotine transformation activity was obtained by growing the mutant in glucose–ammonium–HSP medium. The product was easily purified by dichloromethane extraction. In summary, we developed a novel green route for synthesizing the valuable chemical 6-hydroxynicotine from nicotine and providing an alternative strategy for utilizing tobacco and its wastes.
Bacterial strain, plasmids, and culture conditions
All bacterial strains, vectors, and recombinant plasmids in this study are listed in Table 2. A. tumefaciens S33, deposited at the China center for type culture collection (CCTCC) under accession number CCTCC AB 2016054 (originally CCTCC M 206131), was grown in “nicotine medium” or “nicotine–glucose–ammonium medium” (nicotine medium plus 1.0 g L−1 glucose, 0.2 g L−1 ammonium sulfate, and 1.0 g L−1 yeast extract) at 30 °C, as described previously [11, 35]. Nicotine was added to the media with a final concentration of 1.0 g L−1. 6-Hydroxynicotine medium and HSP medium contain 0.5 g L−1 6-hydroxynicotine or HSP instead of nicotine in the nicotine medium, respectively, as the sole sources of carbon and nitrogen. E. coli cells were routinely grown in LB medium (10.0 g L−1 tryptone, 5.0 g L−1 yeast extract, and 10.0 g L−1 NaCl, pH 7.5) at 37 °C. Nicotine (> 99%) was obtained from Fluka (Buchs, Switzerland). HSP was purified from the culture broth of the nicotine-degrading P. putida S16 as described . Authentic 6-hydroxynicotine was bought from Toronto Research Chemicals, Inc. (Toronto, Canada). All other chemicals were commercially available. The antibiotics and concentrations used were as follows: ampicillin (Ap), 100 mg L−1; gentamicin (Gm), 50 mg L−1.
All assays were carried out in quartz cuvettes (1-cm light path) filled with 1 mL of reaction mixture at 30 °C using a UV–visible Ultrospec 2100 pro Spectrophotometer (GE Healthcare, USA). The reactions were initiated by the addition of enzyme. Ndh activity was determined as previously described  by monitoring the reduction of 2,6-dichlorophenolindophenolsodium (DCIP) with nicotine at 600 nm (ε = 21 mM−1 cm−1). The assay mixture contained 1 mM nicotine, 0.05 mM DCIP, and 50 mM phosphate buffer (pH 7.0). Hno activity was measured by detecting the formation of 6-hydroxypseudooxynicotine as previously reported . The assay mixture contained 0.56 mM 6-hydroxynicotine, 100 mM NaCl, and 100 mM glycine–NaOH buffer (pH 9.2). The formation of 6-hydroxypseudooxynicotine was followed at 334 nm (ε = 20.7 mM−1 cm−1). One unit (U) of enzyme activity was defined as the amount of enzyme catalyzing the conversion 1 µmol of substrate per minute. Protein concentration was measured using the Bradford assay with bovine serum albumin as the standard .
Purification of Hno from A. tumefaciens S33 and identification of its encoding gene
Cells were grown in nicotine–glucose–ammonium medium and disrupted by sonication according to the procedure for purifying NdhAB . During the purification of NdhAB using DEAE Sepharose Fast Flow (GE Healthcare) , three yellow-colored fractions were eluted with 0.25 M NaCl concentration adjacent to the fractions containing NdhAB activity and were found to present Hno activity. The fractions with Hno activity were concentrated, desalted with 50 mM phosphate buffer (pH 7.0), and applied to a Q Sepharose column (GE Healthcare) equilibrated with 50 mM phosphate buffer (pH 7.0). The column was eluted at a 4-mL min−1 flow rate with five column volumes of the same buffer containing 0.1, 0.2, 0.25, 0.4, and 0.5 M NaCl as step gradients. Hno activity was eluted with NaCl of 0.25 M. After being concentrated and desalted, the enzyme was analyzed by SDS-PAGE. The purified enzyme was digested with trypsin and analyzed using MALDI-TOF MS analysis as described . The results were searched against the genome of A. tumefaciens S33  to identify the potential encoding genes of Hno.
Heterologous expression and purification of Hno
The hno gene was amplified by PCR using the genomic DNA of strain S33 as the template. PCR primers (hno-F and hno-R, Table 3) were designed to incorporate restriction sites (BamHI/HindIII) for subsequent ligation into an expression vector. The PCR products were then digested by BamHI and HindIII and ligated into the expression vector pETDuet-1, which was then transformed into E. coli BL21 (DE3) for expression. The recombinant E. coli BL21 (DE3) strains were grown in LB at 37 °C to an optical density of 0.4–0.6 at 620 nm, and the induction was initiated by supplementing with 0.1 mM isopropyl-β-d-thiogalactopyranoside (IPTG) at 16 °C. After incubation for 12 h, cells were harvested and disrupted by sonication. The His-tagged protein was purified using a 5 mL HisTrap HP column (GE Healthcare). The target protein was eluted with a linear gradient of imidazole ranging from 50 to 200 mM in 20 mM NaH2PO4 (pH 7.0) buffer. To remove contaminants, active fractions were further applied to a DEAE Sepharose column that was washed with two column volumes of 50 mM phosphate buffer (pH 7.0) and then eluted with the same buffer containing 0.1, 0.2, 0.3, and 0.5 M NaCl by step gradients (two column volumes per each step). Hno activity was eluted with 0.2 M NaCl. The purity of the protein was detected by SDS-PAGE.
Determination of the enzymatic reaction products
To identify the reaction products catalyzed by Hno, purified Hno was mixed with 11.2 mM 6-hydroxynicotine and 0.2 M NaCl in 1 mL of 50 mM phosphate buffer (pH 7.0) instead of glycine–NaOH because glycine produces an absorption peak in HPLC analysis, causing a negative effect on products separation. The reaction mixture was incubated at 37 °C for 30 min. The reaction was monitored by a UV–visible Ultrospec 2100 pro Spectrophotometer (GE Healthcare). The final products were identified by liquid chromatography-mass spectrometry (LC–MS) as described . LC–MS data were obtained using a Finnigan Surveyor MSQ single quadrupole electrospray ionization mass spectrometer coupled with a Finnigan Surveyor HPLC (Finnigan/Thermo Electron Corporation, San Jose, CA, USA). Positively charged ions were detected. The HPLC system was equipped with an Agilent Eclipse XDB-C18 column (column size, 250 × 4.6 mm; particle size, 5 µM; Agilent, USA) and a PDA detector. A mixture of methanol and 12 mM formic acid (10:90, v/v) was used as the mobile phase, and the flow rate was set at 0.5 mL min−1.
Deletion and complementation of the hno gene
The deletion of the hno gene was performed using the in-frame deletion system based on homologous recombination . First, a 503-bp upstream sequence (primers A and B in Table 3) and a 485-bp downstream sequence (primers C and D in Table 3) were amplified by PCR using the genome of A. tumefaciens S33 as template. The PCR products above were mixed together for another seven amplifying cycles to obtain truncated hno genes due to the 19-bp complementary sequences between primers B and C. The truncated hno genes were used as a template for the third PCR to procure more of the shortened target genes and were then inserted into the suicide plasmid pJQ200SK with restriction sites BamHI and ApaI, generating the recombinant plasmid pJQ-∆hno. The recombinant plasmid pJQ-∆hno was transferred into A. tumefaciens S33 by conjugation with the help of E. coli HB101(pRK2013). The mutant with single-crossover DNA exchange was obtained by the Gm-resistance screening. After culturing the mutant in HSP medium containing 20% sucrose (w/v), double-crossover DNA exchange was achieved, and the plasmid pJQ200SK with completed hno gene was removed, generating A. tumefaciens S33-∆hno which is sensitive to Gm.
To recover the activity of Hno for A. tumefaciens S33-∆hno, the complete hno genes were amplified from the genome of A. tumefaciens S33 using the primers F2 and R2 (see Table 3). The PCR products were digested by ApaI and BamHI and inserted into the plasmid of pBBR1MCS-5 with the same restriction sites to procure the complementation plasmid pBBR-hno. Then the recombinant plasmid was transferred into A. tumefaciens S33-∆hno through electroporation transformation (100 μL competent cells, 1 μg plasmid DNA, 1.2 kV cm−1 field strength, 200 Ω resistance, 25 μF capacitance, Bio-Rad Gene Pulser Xcell™ system, Hercules, CA, USA) , obtaining the complementation strain A. tumefaciens S33-∆hno-C.
To further confirm the deletion of the hno gene, the wild-type strain A. tumefaciens S33, and the engineered strains, A. tumefaciens S33-∆hno and A. tumefaciens S33-∆hno-C, were cultured in LB, HSP, nicotine, and 6-hydroxynicotine media. For LB, HSP, and nicotine media, optical density (OD) at 620 nm was measured. For 6-hydroxynicotine medium, a solid agar plate was used to observe cell growth. Then the three strains were cultured in HSP medium or nicotine–glucose–ammonium medium. Cells were collected by centrifugation at 30,000×g for 10 min and disrupted by sonication. The Ndh and Hno activities were determined, as described above.
Extraction of crude nicotine from tobacco waste
The nicotine used as the substrate for the biotransformation reactions in this study was prepared from tobacco waste according to a previous report . The tobacco waste containing 2.3% (w/w) nicotine was obtained from the Yuxi Cigarrette Co. Ltd., Yunnan Province, China. Nicotine was separated by steam distillation, purified by extraction with chloroform, and then evaporation was used to recover the solvent. The final product contained 94–97% nicotine.
Test of the reaction catalyzed by the whole cells of A. tumefaciens S33-∆hno
To test the possibility of biotransformation of nicotine into 6-hydroxynicotine, the whole cells (~ 1.45 g L−1 DCW) of A. tumefaciens S33-∆hno were used as a catalyst. These cells were prepared by growing in nicotine–glucose–ammonium medium for 24 h. The reaction was performed at 30 °C in 50 mM sodium phosphate buffer (pH 7.0) with 0.85 g L−1 nicotine as the substrate. Concentrations of nicotine and the expected product 6-hydroxynicotine were determined by HPLC (Agilent 1100 system, equipped with an Eclipse XDB-C18 column and a PDA detector). The mobile phase included methanol and 8 mM formic acid (10:90, v/v) with a flow rate of 0.5 mL min−1 at 30 °C.
Optimization of the reaction conditions for the biotransformation of nicotine into 6-hydroxynicotine by whole cells of A. tumefaciens S33-∆hno
To improve the catalytic rate to produce 6-hydroxynicotine, different reaction conditions were examined. Routinely, the reactions were carried out at 30 °C in 50 mM sodium phosphate buffer (pH 7.0) with 1.0 g L−1 nicotine as the substrate and ~ 1.5 g L−1 DCW whole cells of A. tumefaciens S33-∆hno as a catalyst, which were grown in nicotine–glucose–ammonium medium for 24 h. The examined reaction conditions were as follows: The amount of A. tumefaciens S33-∆hno whole cells used for the catalyst was tested in a range from 0.3 to 4.8 g L−1 DCW. The tested initial concentration of nicotine increased from 1 to 16 g L−1. The buffers used were changed from pH 6.0 to 10.0, where 50 mM sodium phosphate buffer (pH 6.0 and pH 7.0), 50 mM Tris–HCl buffer (pH 8.0), and 50 mM glycine–NaOH buffer (pH 9.0 and pH 10.0) were prepared. The catalytic temperature varied from 16 °C to 44 °C. The oxygen requirement was tested in a rotary shaker with the rotation speed set at 0, 100, 200, or 250 rpm. Moreover, to obtain the biocatalyst with the highest activity, various media were tested for growing A. tumefaciens S33-∆hno including HSP medium, glucose–ammonium medium, LB medium, and all these media plus 0.1 g L−1 of HSP or nicotine. The amounts of the substrate and product in the reaction mixtures were measured by HPLC as above.
Batch and fed-batch biotransformation
To re-utilize the biocatalyst, batch and fed-batch biotransformation were tried. Cells of A. tumefaciens S33-∆hno (~ 1.0 g L−1 DCW), cultured with glucose–ammonium medium plus 0.1 g L−1 HSP, were added as a catalyst to 200 mL of 50 mM sodium phosphate buffer (pH 7.0) containing 1.0 g L−1 nicotine. The reaction was performed at 30 °C with a speed of 200 rpm. For the batch biotransformation, the biocatalyst was recycled by centrifugation to collect the cells and then was re-used three times. For the fed-batch biotransformation, nicotine was supplemented three times at a concentration of 1.0 g L−1 after the substrate was almost completely consumed.
Extraction and purification of the product 6-hydroxynicotine
After the reaction finished, the supernatant was obtained by centrifugation at 10,000×g for 10 min and adjusted to pH 10.5 with 2 M NaOH. Then the supernatant was concentrated by rotary evaporation under reduced pressure at 60 °C. The product 6-hydroxynicotine was extracted from the concentrate with equal volume of dichloromethane for three times. The extracts were pooled, and then was dried using Na2SO4. The solvent was removed further by evaporation. The isolated product was identified by recording the UV–visible absorption spectra after being dissolved in a 0.1-M HCl solution and determining its mass spectrometry by LC–MS on the Dionex’s UltiMate 3000 UHPLC-Bruker’s impact HD high-resolution mass spectrometry system. The same column and chromatography conditions used above were applied. The NMR spectra were recorded for solutions in CDCl3 on an AVANCE 600 spectrometer (Bruker, Switzerland) operating at 600 MHz for 1H and at 150 MHz for 13C.
Nucleotide sequence accession numbers
The A. tumefaciens S33 genome GenBank accession numbers are CP014259.1 and CP014260.1.
dry cell weight
fragments per kilobase per million
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SW, WY, HH, and HX designed the experiments, analyzed the data, and wrote the manuscript. WY, RW, HL, JL, and YW performed the experiments. All authors discussed the results and commented on the manuscript. All authors read and approved the final manuscript.
We thank Professor Ping Xu from Shanghai Jiao Tong University for his valuable supports. We also thank Caiyun Sun, Jing Zhu, and Zhifeng Li from Analysis and Testing Center of SKLMT (State Key Laboratory of Microbial Technology, Shandong University) for assistance in HPLC and LC–MS analyses. This work was supported by the grant from the Fundamental Research Funds of Shandong University (Grant No. 2014JC023).
The authors declare that they have no competing interests.
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About this article
- 6-Hydroxynicotine oxidase
- Functionalized pyridine
- Tobacco wastes
- Agrobacterium tumefaciens