- Original article
- Open Access
The first fungal laccase with an alkaline pH optimum obtained by directed evolution and its application in indigo dye decolorization
AMB Express volume 9, Article number: 151 (2019)
Engineering of fungal laccases with optimum catalytic activity at alkaline pH has been a long-lasting challenge. In this study, a mutant library containing 3000 clones was obtained by error-prone PCR to adapt the optimum pH of a fungal laccase Lcc9 from the basidiomycete Coprinopsis cinerea. After three rounds of functional screening, a mutant with three amino acid changes (E116K, N229D, I393T) named PIE5 was selected. PIE5 showed an optimum pH of 8.5 and 8.0 against guaiacol and 2,6-DMP when expressed in Pichia pastoris, representing the first fungal laccase that possesses an optimum pH at an alkaline condition. Site directed mutagenesis disclosed that N229D contributed the most to the optimum pH increment. A single N229D mutation caused an increase in optimum pH by 1.5 units. When used in indigo dye decolorization, PIE5 efficiently decolorized 87.1 ± 1.1% and 90.9 ± 0.3% indigo dye at the optimum conditions of pH 7.0–7.5 and 60 °C, and with either methyl 3,5-dimethoxy-4-hydroxybenzoate or 2,2′-azino-bis(3-ethylbenzothazoline-6-sulfonate) as the mediator. In comparison, the commercially available fungal laccase TvLac from Trametes villosa decolorized 84.3 ± 1.8% of indigo dye under its optimum conditions (opt. pH 5.0 and 60 °C). The properties of an alkaline-dependent activity and the high indigo dye decolorization ability (1.3-fold better than the parental Lcc9) make the new fungal laccase PIE5 an alternative for specific industrial applications.
Laccases (benzenediol: oxygen oxidoreductases, EC 22.214.171.124) are a family of copper-containing oxidases (Baldrian 2006). They consist of three cupredoxin domain repeats D1 to D3 and contain four copper atoms as cofactors in two distinctive sites, with a type I copper center (T1) located in the core of D3, and a type II/type III trinuclear copper cluster (T2/T3) situated in a surface exposed cleft in between D1 and D3 (Hakulinen and Rouvinen 2015). Laccases can oxidize a variety of phenolic and non-phenolic substrates with or without mediators (Baldrian 2006). When oxidizing the substrate, electrons transfer from the substrate to the T1 Cu, then from the T1 site to the trinuclear copper cluster T2/T3, and eventually to a dioxygen molecule bound between the two T3 copper ions (Jones and Solomon 2015). Due to their strong oxidative power and with water as the final by-product, laccases are regarded as versatile enzymes for biotechnical applications such as pulp bleaching, textile refining, food upgrading, biofuel production, organic compound synthesis, bioremediation, and protective agents in cosmetics (Pezzella et al. 2015; Sitarz et al. 2016).
Laccases are widely distributed over bacteria, fungi, insects, and plant kingdoms (Hoegger et al. 2006; Kües and Rühl 2011). However, most of the laccases characterized until now are of bacterial or fungal origin due to their ease of production and purification (Baldrian 2006; Chauhan et al. 2017). Typically, bacterial laccases have a low-redox potential (340–470 mV), while their fungal counterparts have middle- (490–710 mV) and high-redox potentials (730–790 mV) (Rodgers et al. 2010; Mate and Alcalde 2015). The higher redox-potential and specific activity, and a broader substrate spectrum of fungal laccases make them much more attractive in terms of specific industrial applications than the corresponding bacterial laccases (Rodgers et al. 2010; Pezzella et al. 2015).
One of the most intriguing characteristics of fungal laccase catalysis is its pH dependence. Most fungal laccases display toward phenolic substrates an optimum activity in the pH range of 3.0–5.5 and they become essentially inactive as the pH is approaching to neutral and alkaline, although they are structurally stable above 7.0 (Xu 1997; Baldrian 2006). On the other hand, fungal laccases with high activity at neutral/alkaline pH are highly desirable, especially for their applications in specific industrial processes (Madzak et al. 2006; Torres-Salas et al. 2013; Novoa et al. 2019). For example, during a bioethanol production process using steam-exploded wheat straw as the substrate, treatment with laccase at alkaline condition (pH 8) resulted in a reduction in lignin content in the solid fraction and in an increase in both glucose and xylose production after a saccharification step (De La Torre et al. 2017). Alkaline-tolerant (pH 9) laccase is more preferred in hair coloring industries (Endo et al. 2012; Fang et al. 2014). Furthermore, fungal laccases with high activity at blood pH (pH 7.4) also show potential to contribute to the technology revolution of implantable self-contained wireless 3D nano-biodevices that work in different physiological fluid (Mate et al. 2013a). At the present time, the main technological applications of fungal laccases are still in the textile industries, for example in eco-friendly denim destaining (Pezzella et al. 2015; Muñoz et al. 2017). Experience showed that degradation of indigo dye by alkaline active fungal laccases (pH > 7) results in less background staining of jeans as compared with the practice conducted in acidic conditions. Destaining at neutral pH could thus provide products with better added-values (Colomera and Kuilderd 2015). Unfortunately, no effective fungal laccases with optimum pH at neutral/alkaline conditions have been reported from nature and could so far neither be created in the laboratory despite of much efforts of mutagenesis (Maté et al. 2010, 2013a, b; Mate and Alcalde 2015; Novoa et al. 2019).
Previously, we obtained a laccase named Lcc9 from the basidiomycete Coprinopsis cinerea (Pan et al. 2014) which is naturally expressed by the fungus (in the further called wLcc9 for wild-type Lcc9) upon induction by p-hydroxybenzoic acid (HBA) (Hu et al. 2019). Lcc9 recombinantly produced in Pichia pastoris (rLcc9) showed an optimum pH of 6.5 towards phenolic substrates such as guaiacol after heterologous expression in P. pastoris (Xu et al. 2019). In this study, error-prone PCR and screens in P. pastoris were used for directed protein mutagenesis to increase the laccase activity of Lcc9 in alkaline pH. One positive mutant enzyme (designated as PIE5) with an optimum pH of 8.5 towards guaiacol was obtained. The application potential of PIE5 on indigo dye decolorization was also evaluated. PIE5 represents the first fungal laccase with an alkaline pH optimum and can serve as candidate for specific applications at alkaline conditions.
Materials and methods
Strains, chemicals, and culture media
Escherichia coli JM109, P. pastoris GS115 and the plasmid pPIC9K were purchased from Invitrogen (Carlsbad, CA, USA). Guaiacol, 2,6-dimethoxyphenol (2,6-DMP), and 2,2′-azino-bis(3-ethylbenzothazoline-6-sulfonate) (ABTS) were obtained from Sigma-Aldrich (St. Louis, MO, USA). The error-prone PCR kit was acquired from Aviva Systems Biology (Beijing, China). All other chemicals and reagents were of analytical grade. Yeast Extract Peptone Dextrose Medium (YPD), Minimal Dextrose Medium (MD), Buffered Glycerol-Complex Medium (BMGY) and Buffered Minimal Methanol Medium (BMM) were prepared following the instructions from Invitrogen.
Mutation library construction and screening
Error-prone PCR based mutagenesis was conducted using a cloned lcc9 cDNA sequence as the template and a primer pair of lcc9F and lcc9R as primers (Xu et al. 2019) (Additional file 1: Table S1). The final MnCl2 concentrations in the amplification system were 0.6, 0.7, 0.8, 0.9, and 1.0 mM, respectively. The mutated cDNA fragments amplified by the PCR were recovered, mixed together, digested with NotI and EcoRI, and ligated into the pPIC9K vector subjected to the same digestion treatment, generating a library of plasmids pPIC9K-mlcc9 with mutated lcc9 cDNA fragments. The pPIC9K-mlcc9 library was transformed into competent E. coli JM109 cells and screened using Amp. All Amp-resistant E. coli JM109 clones were harvested and plasmids were extracted, which were then linearized by using SacI and transformed into P. pastoris GS115 by electroporation. The electroporated cells were plated onto MD agar plates for selecting the His+ transformants. All transformants were selected and grown on BMGY plates at 28 °C for 2 days and kept at − 80 °C as a mutation library for future usage. P. pastoris GS115 transformed with the empty vector pPIC9K (P. pastoris GS115/pPIC9K) and pPIC9K-lcc9 with the original lcc9 cDNA (P. pastoris GS115/pPIC9K-lcc9) were used as negative and positive controls in the following screenings.
For the first-round screening, the strains were cultivated for 4 days at 28 °C on BMMC agar plates containing 0.2 mM ABTS. Secretion of active laccase, with methanol induction, was identified by the presence of a dark green zone around transformant colonies. Positive clones were selected and in second-round screening cultivated for 48 h at 28 °C in shaken 96-well plates (200 rpm) containing 50 μL BMGY medium in each well. Then, 150 μL liquid BMM medium was added into each well to induce laccase expression. After incubating at 28 °C and 200 rpm for another 48 h, the plates were centrifuged at 2500×g for 5 min to obtain the supernatants, which were transferred into new plates for laccase activity determinations. The assay system for the second-round screening contained citrate/phosphate buffer (pH 6.5 or 8.5) and 10 mM guaiacol in a total volume of 200 μL added to each well. The absorbance was monitored at 465 nm and 30 °C for 10 min. Mutants with higher activity at pH 8.5 than at pH 6.5, and with higher activity at pH 8.5 than the positive control P. pastoris GS115/pPIC9K-lcc9 were selected for further screening. In the third-round screening, positive colonies were cultured in shaking flasks, enzyme expression was methanol-induced and mutant proteins were purified to homogeneity as described in Xu et al. (2019) for optimum pH determination.
Specific mutants of Lcc9 were constructed based on site-directed mutagenesis using respective primers (Additional file 1: Table S1) and the plasmid pPIC9K-lcc9 as the template (Xu et al. 2019). Positive P. pastoris strains harboring the intended mutant genes were obtained as described above and verified by sequencing.
Laccase expression and purification
Laccase expression in P. pastoris was conducted according to Xu et al. (2019). The wild-type Lcc9 (wLcc9; GenBank: DAA04514.1) expressed by C. cinerea was obtained by cocultivation C. cinerea Okayama 7 with Gongronella sp. w5 and purified according to the method of Pan et al. (2014).
When purifying rLcc9 and mutant laccases, the aqueous culture broth was centrifuged at 8000×g for 10 min. Culture supernatants were collected and concentrated to 100 mL in a Minitan Ultrafiltration System with a regenerated low-binding cellulose membrane (Millipore, Bedford, MA, USA). The concentrate was centrifuged at 12,000×g for 20 min, and the supernatant was then dialyzed against citrate/phosphate buffer (20 mM, pH 7.5) overnight, followed by centrifugation again at 12,000×g for 20 min. Then, the supernatant was applied to a DEAE-Sepharose FF column (10 × 200 mm, Amersham Pharmacia, Uppsala, Sweden) and eluted according to protocols reported previously (Xu et al. 2019).
The homogeneity of the purified protein was determined by sodium dodecyl sulfate (SDS) polyacrylamide gel electrophoresis (PAGE) with a 12% polyacrylamide gel and stained with Coomassie Brilliant Blue R-250. The protein concentration was assayed using the Bradford method, with bovine serum albumin as standard (Sangon Biotech, Shanghai, China). Native PAGE was conducted using guaiacol as the substrate as described previously (Pan et al. 2014). The purified laccase was identified according to Rühl et al. (2013) by LC–ESI–MS/MS (LTQ, Thermo Fisher Scientific, Shanghai, China). Proteins were then identified by searching the data against a database of the C. cinerea Okayama 7 (#130) (Stajich et al. 2010).
The assay mixture consisted of 10 μL of appropriately diluted culture supernatant or enzyme stock and 990 μL of 100 mM citrate/phosphate buffer (pH 4.0) containing 5 mM guaiacol. It was measured at 465 nm for 5 min at 30 °C (ε465 = 12,000 M−1 cm−1) (Froehner and Eriksson 1975). Alternative substrates for the measurement of laccase activity were 0.5 mM ABTS (ε420 = 36,000 M−1 cm−1) (Paice and Bourbonnais 1990) and 10 mM 2,6-DMP (ε468 = 49,600 M−1 cm−1) (Fang et al. 2015). Heat-treated laccase was used as the control. One activity unit (U) was defined as the amount of laccase protein required for oxidizing 1 μmol of substrate per minute. All experiments were performed in triplicate.
Characterization of mutant laccases
The effect of pH on laccase activity was assayed in 50 mM citrate/phosphate buffer (4.0–8.0) and 50 mM Tris/HCl buffer (8.0–9.5) at 60 °C. The effect of temperature was determined by incubating protein in the temperature range of 4–80 °C at the optimum pH for each substrate. The enzyme stabilities against pH and temperature were determined by incubating proteins at various temperatures and different pH values, and then the residual activities were determined as mentioned above. All experiments were performed in triplicate.
The kinetics and the specific activities toward guaiacol and 2,6-DMP of rLcc9 and the seven distinct mutants created in this study were measured at the optimum pH and temperature of each mutant. The kinetic constants (Km, kcat, and kcat/Km) were determined by incubating proteins with various concentrations of guaiacol and 2,6-DMP.
The redox-potential of laccases was measured using cyclic voltammetry at pH 6.5. The pyrolytic graphite electrode (PGE, GaossUnion, Shanghai, China), platinum wire electrode (ChenHua, Shanghai, China), and calomel electrode (ChenHua) were used as the working electrode, counter electrode, and reference electrode, respectively. Before testing, the PGE was prepared by ultrasonic cleaning for 5 min with 95% ethanol and H2O, respectively. Then, 5 μg laccase was dripped on the PGE and placed at 4 °C until the laccase was completely adsorbed on the PGE. Then, the redox potentials of the samples were detected using an electrochemical workstation (CHI660D, Chenhua, China).
Sequence alignment and protein structure modeling
The most similar protein to PIE5 was a laccase (Lcc4) from Lentinus sp. that has 56% sequence identity (PDB id:3X1B) to C. cinerea wLcc9 (GenBank: DAA04514.1) with its crystal structure resolved at 1.8 Å (Maestre-Reyna et al. 2015). A PIE5 model was thus generated by using the automated Swiss-Model protein modeling server and Lentinus Lcc4 as the template (http://swissmodel.expasy.org/) and analyzed with the PyMol software.
Indigo dye decolorization
The mutant PIE5, wLcc9, and rLcc9 were used for indigo dye (Sigma-Aldrich) decolorization. Initially, the test system contained citrate/phosphate buffer (50 mM, pH 7.0), enzyme (200 mU mL−1), and indigo dye (200 μM) in a total volume of 1 mL. The reaction mixtures were incubated at 40 °C (except for temperature optimization reactions) for 2 h. Mediators (final concentration, 100 μM) including 3,5-dimethoxy-4-hydroxybenzaldehyde (DHB), syringic acid (SA), methyl 3,5-dimethoxy-4-hydroxybenzoate (MS), 1-hydroxybenzotriazole (HBT), and ABTS were used to evaluate the effect of mediator on decolorization. The effects of pH (4.5–9.0), temperature (20–80 °C), mediator concentration (20–300 μM), reaction time (0–180 min), and enzyme concentration on dye decolorization (40–200 mU mL−1) were evaluated one by one based on a single factor optimization strategy. All assays were carried out in triplicate. The decolorization rates of indigo dye by laccases were monitored according to the decrease in absorbance at 665 nm. The heat-treated enzymes were used as the negative controls.
Reactions using the commercial fungal laccase from Trametes villosa (Tlac, provided by Novozymes, Tianjin, China) were used as the positive controls. Briefly, when 200 μM ABTS was used as the mediator, the test system contained 200 mU mL−1 Tlac and 200 μM indigo dye in a total volume of 1 mL. Reaction was conducted at pH 7.0 and 60 °C for 180 min. When 120 μM MS was used as the mediator, reaction was conducted at pH 7.5 and 60 °C for 50 min. Meanwhile, reaction was also conducted at pH 5.0 and 60 °C for 3 h according to the manufacturer’s instruction, without addition of any mediator.
The decolorization ratio was calculated according to the following equation
A0 and A represent the initial and final absorbance of indigo dye, respectively.
Laccase mutation library construction and positive clone screen
Lcc9 cDNA was previously successfully expressed in P. pastoris (Xu et al. 2019). It was used as the template for directed evolution to improve the pH optimum of Lcc9 to alkaline condition. Based on the error-prone PCR technique, a Lcc9 cDNA mutation library was obtained which contained 3000 P. pastoris colonies with an average mutation rate of 4.63 nucleic acids per gene copy, according to the sequencing of 60 randomly picked colonies (data not shown).
Phenotype analysis was used to select the target mutants in the first-round functional screening. A total of 1960 colonies, which showed a dark-green halo around the colony after 4 days cultivation on the BMMC agar plates of stronger intensity than the control with plasmid pPIC9k were recognized as positive colonies and picked up for future screening. In the second-round multi-well plate screening, four positive colonies with at least 10% higher laccase activity at pH 8.5 than at 6.5 and at least 10% higher activity at pH 8.5 than the control rLcc9 colony were screened out based on activity determination using guaiacol as the substrate. In the third-round liquid fermentation screening, one mutant protein, named PIE5, with an optimum pH of 8.5 was obtained. PIE5 retained more than 70% of original activity in the pH range of 7.0–9.5 (Fig. 1). In comparison, rLcc9 showed an optimum pH of 6.5 and retained approximately 60% of the original activity in the pH range of 5.0–8.0 (Fig. 1 and Xu et al. 2019). In the slightly acidic pH range at pH 5.0 to pH 6.5, enzyme activities measured for PIE5 were lower, between ca 20 and 55% of optimum activity.
Biochemical property comparison between PIE5 and rLcc9
PIE5 showed an optimum catalytic temperature at 60 °C (Table 1), which was the same to that of rLcc9 (Xu et al. 2019). However, the temperature and pH stabilities of the PIE5 were quite different from those of rLcc9. Generally, rLcc9 was more stable than PIE5 both at pH 6.5 and 8.5 and at temperatures of 50 °C and 60 °C, respectively (Fig. 2). At 50 °C, PIE5 was more stable at pH 8.5 than that at 4.5 and 6.5, with 65% of the original activity that retained after 1 h incubation at pH 8.5. PIE5 showed a half-life time of 20 min and 30 min, respectively, after incubation at 60 °C and pH 8.5 and 6.5. In comparison, rLcc9 retained more than 85% of activity after 1 h incubation at 50 °C and pH 6.5 and 8.5, and it retained more than 60% of activity after 1 h incubation at 60 °C and pH 6.5 and 8.5 (Fig. 2). These results suggested that PIE5 showed a strong reduction in both its thermostability and pH stability as compared to rLcc9.
The specific activity of PIE5 was 318.4 U mg−1 towards ABTS, comparable to that of rLcc9 (315.3 U mg−1, Xu et al. 2019). The kinetic properties of PIE5 and rLcc9 were determined under optimum conditions (Table 1). When using guaiacol and 2,6-DMP as the substrates, the Km of PIE5 increased 3.7-fold (3.3 × 10−4 M) and 2.5-fold (5.7 × 10−3 M), compared to those of rLcc9, which were 0.9 × 10−4 and 2.3 × 10−3 M, respectively. PIE5 showed a 2.8-fold increase in kcat on guaiacol compared to that of rLcc9. This result translated to a similar catalytic efficiency of PIE5 compared to that of rLcc9. In comparison, when using 2,6-DMP as a substrate, PIE5 showed a 1.6-fold decrease in kcat, resulting in a fourfold decrease in catalytic efficiency as compared to that of rLcc9 (Table 1). The better performance of PIE5 against guaiacol than against 2,6-DMP may be attributed to the fact that guaiacol was used as the selection substrate throughout the screening process (Madzak et al. 2006).
Sequence analysis of PIE5
PIE5 contained three mutations in the sequence, including E116K, N229D, and I393T. Sequence alignment was conducted among C. cinerea Lcc9 and other fungal laccases with known structures presented in the PDB database. Inspection of the sequence alignments of the laccase family revealed that the position 116 is located between the two laccase signature regions L1 and L2 for copper-binding (Kües and Rühl 2011) including the consensus motifs VN(T)QCPI and WYHSH. Furthermore, position 116 is quite variable in laccase sequences: L, S, or D are the main residues that occur at this position. In comparison, E is present in Lcc9 at this position (Additional file 1: Fig. S1). Differently from the loop region with E116 in between L1 and L2, the positions 229 and 393 are highly conserved among laccases from basidiomycetes. For example, position 393 in Lcc9 is occupied by an I, which is not found in many other laccases at the same position (Additional file 1: Fig. S1) while e.g. in some putative laccases from related species of the Psathyrellaceae family (not further shown). As an alternative, a V is often encoded at this position in other fungal laccase genes of other families of Basidiomycetes (Additional file 1: Fig. S1).
Homology modeling of the PIE5 structure was employed using the laccase from Lentinus sp. (PDB ID: 3X1B, 56% sequence identity to the wild-type Lcc9) as a template to further understand the contribution of the three potentially beneficial mutations in PIE5 (Maestre-Reyna et al. 2015). The three mutated sites were distributed over different domains of the protein. Accordingly, E116K and I393T were both located on the surface of the protein, and were far from the substrate binding area, the copper centers, and the water channel, respectively (Fig. 3a). However, the negatively charged E116 on the laccase domain D1 of the wildtype Lcc9 enzyme was H-bonded with the polar S501 from the laccase domain D3, suggesting that they may contribute to a pH-dependent 3-dimensional stability of the protein by the formation of interdomain bridges (Herrera-Zúñiga et al. 2019). After the substitution to the positively charged K, the H-bond was abolished (Fig. 3c, d and Additional file 1: Fig. S2).
I393T was located on the first loop region that connects the β-sheet on D3 (Fig. 3). No convincing structural or interaction change was found for I393T with the change from the hydrophobic I to the polar T (Fig. 3 and Additional file 1: Fig. S2). However, five transportation channels (P1–P5) were recently predicted based on the random acceleration molecular dynamic simulations (Li and Zhao 2018). Based on the PIE5 model, I393T was located close to the oxygen entrance of channel P1 (Fig. 3b), which is recognized as the oxygen channel with the highest efficiency (Piontek et al. 2002). As a result, we deduced that I393T may affect the oxygen transfer from the outside to the T3 Cu2+.
N229D was found in a random coil of the notch inside of the protein in D2 (Fig. 3a). Position 229 may participate in the formation of the optimal binding pocket for a specific substrate (Pardo et al. 2016; Mehra et al. 2018). In the wildtype Lcc9, N229 interacted with the surrounding residues Q258, I259 and N285 through a complex network of H-bonds (Fig. 3c, d). After mutation, except for N285, the H-bonds of D229 with the surrounding residues Q258 and I259 were abolished. Meanwhile, D229 formed a new H-bond with A261, which was located near the T2/T3 copper center (Fig. 3c, d). It seems that a new linkage was made as follows: D229-A261-G262-W129-H87-T2/T3 copper center, which means that the mutation N229D may indirectly affect the T2/T3 copper center (Additional file 1: Fig. S2).
Characterization of the three PIE5 mutations in single and double mutants
Six different mutants, namely E116K, N229D, I393T, E116K/N229D, E116K/I393T, and N229D/I393T, were constructed based on site-directed mutations. They were expressed in P. pastoris, purified, and biochemically characterized following the protocols as described in “Materials and methods” section (Table 1 and Additional file 1: Fig. S3).
Biochemical characterization showed that the six mutated proteins showed different optimum pHs. Among them, E116K and E116K/I393T showed an optimum pH of 6.5 toward guaiacol, similar to that of rLcc9, indicating that position E116K had little impact on increasing the optimum pH to alkaline. N229D contributed the most to the optimum pH increment, because both the single-point mutation N229D and the two-point mutations including N229D each caused a 1.5 units increment in the optimum pH in activity toward guaiacol. I393T showed an optimum pH of 7.0 towards guaiacol. E116K, I393T, and E116K/I393T showed an optimum pH of 7.0 toward 2,6-DMP, compared to 6.5 of rLcc9. In comparison, mutants including N229D, E116K/N229D, and N229D/I393T shared the same optimum pH of 8.0 with that of PIE5 (Table 1). All the six mutants shared the same optimum temperature of 60 °C with rLcc9 and PIE5 (Table 1).
As measured with ABTS, the specific activities were 251.2, 477.9, 173.8, 253.2, 176.5, and 363.3 U mg−1 for E116K, N229D, I393T, E116K/N229D, E116K/I393T, and N229D/I393T, respectively. Under optimum conditions, the kinetic constants of the six mutated proteins were tested and listed in Table 1. I393T and E116K/I393T showed a 2.5 to 3-fold increase in substrate affinity when compared to PIE5, more similar to rLcc9, whereas other mutations showed no apparent changes in substrate affinity toward guaiacol as compared to PIE5. Except for E116K/I393T, which showed a kcat of 46 s−1, other mutants showed kcat values of 75.4 to 87.3 s−1, higher than that of PIE5, which was 62.9 s−1. It should be noted that the catalytic efficiencies of I393T and E116K/I393T were 5.7 × 105 and 3.9 × 105 M−1 s−1, three- and twofold higher than that of PIE5, respectively.
Redox potentials of the proteins
The redox potentials of the proteins mentioned above were tested using a cyclic voltammetry method at pH 6.5. PIE5 showed a redox potential of 598.9 mV, much higher than that of rLcc9, which was 505.7 mV under the same test condition (Table 1). The redox potential of the six mutated proteins were ranged from 515.7 to 582.7 mV, and were lower than that of PIE5, but higher than that of rLcc9 (Table 1).
Indigo dye degradation
PIE5 hardly oxidized indigo dye in the absence of mediator, with only 5% indigo dye that was decolorized after 2 h incubation under initial test conditions (Fig. 4a). Addition of mediators including MS, DHB, SA, HBT, and ABTS promoted the decolorization rates of PIE5 on the indigo dye. MS was the best mediator for decolorization under the initial test conditions. The decolorization rate for PIE5 in the presence of MS was 59.7 ± 3.5%. Using ABTS as the mediator, the decolorization rate was 48.4 ± 2.0%. Mediators to improve indigo dye decolorization by PIE5 were ranked as follows: MS > ABTS > DHB > SA > HBT (Fig. 4a).
The conditions for PIE5 to decolorize indigo dye were further optimized by using a single factor optimization method. PIE5 showed a high decolorization rate at neutral/alkaline conditions. When using MS and ABTS as the mediators, the optimum pH and temperature for PIE5 to decolorize indigo dye were pH 7.5 and 60 °C, and pH 7.0 and 60 °C, respectively (Fig. 4b, c). PIE5 decolorized about 40% of 200 μM indigo dye even at pH 9.0 after incubation at 40 °C for 2 h (Fig. 4b). The performance of PIE5 was positively associated with the mediator dosage (Fig. 4d), PIE5 concentration (Fig. 4e), and incubation time (Fig. 4f). Finally, in the presence of 120 μM MS, 200 mU mL−1 PIE5 decolorized 87.1 ± 1.1% of 200 μM indigo dye after 50 min of incubation at pH 7.5 and 60 °C (Fig. 4f). When using 200 μM ABTS as a mediator, 200 mU mL−1 PIE5 decolorized 90.9 ± 0.3% of 200 μM indigo dye after incubating at pH 7.0 and 60 °C for 3 h (Fig. 4f), which was much better than the performances of wLcc9 and rLcc9, which were 70–72% and 75–79%, respectively, under the same conditions (Table 2).
The performance of PIE5 on indigo dye decolorization was further compared to that of commercial T. villosa laccase from Novozymes. Under the conditions suggested by the producer at pH 5.0, 200 mU mL−1 T. villosa laccase decolorized 84.3 ± 1.8% of 200 μM indigo dye after incubation at 60 °C for 3 h. Furthermore, the T. villosa laccase decolorized 69.6 ± 1.3% and 59.3 ± 1.8% of 200 μM indigo dye, respectively, under the same conditions as optimized for PIE5 (Table 2).
Fungal laccases have been extensively studied over the past decades and recognized as being one of the ‘greenest’ catalysts (Pezzella et al. 2015). However, one of the major obstacles that prevented rapid progress of fungal laccase in applications in modern industries is their acidic pH dependence (Madzak et al. 2006; Torres-Salas et al. 2013; Novoa et al. 2019). This is because most of the fungal laccases show an optimum pH of 3–5.5 over phenolic substrates and they rapidly lose their activities at pH > 7 (Xu 1997; Xu et al. 1998). In consequence, fungal laccases with optimum pH and high activity at neutral or alkaline conditions are highly desirable, especially for applications in specific industrial processes (Madzak et al. 2006; Torres-Salas et al. 2013; Schwaneberg et al. 2018).
Several studies have reported the improvement of the optimum pH of fungal laccases. For example, mutation of basidiomycetous laccase OB-1 resulted in the change of the optimum pH from 4.0 to 5.0–6.0 in reactions with 2,6-DMP as substrate. At pH 7.0, the mutated protein retained 50% of its original activity for 2,6-DMP, whereas the wild-type protein displayed negligible activity under these conditions (Maté et al. 2010). However, all the engineered fungal laccases still have an optimum pH at acidic pHs (Cusano et al. 2009; Mate et al. 2013a, b; Torres-Salas et al. 2013; Novoa et al. 2019), even though one mutant named L365E/L513M of laccase MaL-M1 from Melanocarpus albomyces showed a threefold improved kcat compared to the wild type laccase at pH 9.8 (Novoa et al. 2019). In this study, PIE5, a mutant fungal laccase from C. cinerea with remarkably improved enzymatic activity at alkaline pH, was obtained based on error-prone PCR and high-throughput functional screening. PIE5 showed an optimum pH of 8.5 toward guaiacol, and retained more than 70% of its activity at pH range of 7–9.5 (Fig. 1). Thus, PIE5 is regarded as an efficient catalyst at alkaline conditions. To the best of our knowledge, PIE5 is the first fungal laccase that has an optimum alkaline pH toward guaiacol. The optimum pH of 8.5 is even higher than those of certain bacterial laccases which are well known to have optimum pHs at neutral or slightly alkaline conditions, for example Ibh1 from Bacillus halodurans (optimum pH 7.5–8) (Ruijssenaars and Hartmans 2004), Ppo1 from Marinomonas mediterranea (around pH 7) (Jimenez-Juarez et al. 2005), and Lac15 from a marine metagenome (pH 7.5) (Fang et al. 2011).
According to Xu (1997), both the redox potential difference [ΔE0 = E0 (laccase T1) − E0 (substrate, single electron)] between a reducing substrate and the T1 center, and the OH− inhibition at the T2/T3 center affect the pH activity profile of a laccase towards phenolic substrates: the former positively correlates with the reaction rate and mainly affects the ascending part of the pH profile curve. On the contrary, when the pH increases, the T2/T3 cluster can accept hydroxyl ions, which competes with the ΔE0 contribution, interrupts the trafficking of electrons from T1 Cu, and decreases laccase activity. In this study, both the rLcc9 and PIE5 showed bell-shaped pH profiles toward guaiacol (Fig. 1), indicating that the two physicochemical factors both affect the PIE5 pH profile. From our data, all the mutation proteins showed higher redox potentials than rLcc9 (Table 1), and these connected with the observed optimum pH values of each protein, revealing that the redox potential may be responsible for the optimum pH increment. This may be explained by using Xu’s conclusions: if the redox-potential increases for a laccase, the phenomenon that the enzyme activity decreases during a pH increment may be overcome (Xu 1997; Torres-Salas et al. 2013). However, it should be noted that complex mechanisms other than redox potential also play important roles in the pH effects on fungal laccases against phenol substrates, as indicated in other reports. For example, Cusano et al. (2009) succeeded in shifting the pH profile of a laccase toward an alkaline condition, with which the redox potential of the laccase decreased. In comparison, laccase variant ChU-B exhibits a higher activity at neutral/alkaline pH values than the wild-type laccase from basidiomycete PM1, while keeping the same redox potential (Mate et al. 2013b).
Our results showed that PIE5 contained 3 mutations in the amino acid sequence compared to Lcc9. Based on the biochemical characterization of both single and double mutation proteins, position N229D played the major impact on the pH profile of PIE5 (Table 1). However, mutations at this specific side in laccase have so far not been mentioned in the literature. Position N229 is highly conserved among basidiomycete laccases and located in a conserved random coil of the notch that participates in substrate binding and contributes to the substrate electron transfer (Fig. 3 and Additional file 1: Fig. S2) (Bertrand et al. 2002; Mehra et al. 2018). After the amino acid mutation of N229 to D229, the calculated pI of its side chain changed from 6.3 to 8.6. Usually, amino acids should be freely switched between protonation/deprotonation in a corresponding pH range to facilitate the electron transfer from the substrate to the T1Cu (Shigeno et al. 2015; Magni et al. 2018). In consequence, we suggest that the change from N to D may affect the association/dissociation of amino acids surrounding D229 at pH 8.5, and then substrate recognition guiding and the subsequent substrate electron transmission, as it is also suggested from the altered kinetic values of mutants carrying D229 (Table 1). Indeed, replacing the D with N at position 227 of laccase TvLB from Trametes versicolor changed the optimum pH of the enzyme against 2,6-DMP from pH 3.4 to 4.8, because of favoring substrate deprotonation (Madzak et al. 2006). Moreover, it was reported that the general increase in activity of the variant was due to a conformational rearrangement of the T2/T3 copper coordination sphere (Xu 1997; Mate et al. 2013a; Torres-Salas et al. 2013; Scheiblbrandner et al. 2017). Protein structure assimilation results showed that N229 in wild-type C. cinerea Lcc9 is in complicated manner connected with surrounding residues by using H-bonds (Additional file 1: Fig. S2). The network was changed after the D229 mutation, with some H-bonds abolished and one newly formed. These changes may indirectly affect the microenvironment of the T2/T3 copper center, the election transfer, and OH− binding at the T2/T3 center, and finally this will affect the PIE5 pH profile against substrates such as guaiacol and 2,6-DMP (Table 1).
Other than the N229D mutation, also the single I393T mutation but not the E116K mutation caused a change in the optimum pH on activity against guaiacol by 0.5 units (Table 1). This suggests that also the change I393T will contribute to the change in the optimum pH in PIE5. I393 was found located on the surface of the Lcc9, at long distances to the substrate binding area, the copper centers, and the water channel. No convincing structural changes were found for I393T. However, I393 was found located near the best oxygen transfer channel (Fig. 3b). Given that the dependence of O2 reduction potential on pH could also impact the pH activity profile (Xu 1997), we speculate that the I393T mutation may cause an allosteric effect of PIE5 and affected the transfer of oxygen to the trinuclear copper center, and finally affected the electron transfer from substrate to T1 copper center, T2/T3 center, and to oxygen. As a support to this hypothesis, we found that redox potential of I393T increased to 550.2 mV. The substrate affinities of the three mutants containing I393T also increased 2.5 to 3-folds (Table 1).
Laccases are proteins with highly conserved and functionally essential regions. In consequence, not many positions can be mutated without changing activities (Bloom and Arnold 2009). From structural simulation data, E116 may contribute to formation of interdomain bridges between D1 and D3 (Herrera-Zúñiga et al. 2019). As a result, the identified serendipitous mutation E116K, although not directly involved in catalysis, may be involved in influencing the pH profile of the enzyme by influencing protein structure and stabilization (Maté et al. 2010, 2013a; Scheiblbrandner et al. 2017).
At present, main technological applications of fungal laccases are in the textile industry (Pezzella et al. 2015). They are used in the enzymatic degradation of indigo dye in both the stone-wash process and the deinking treatment of dyeing effluents (Mishra et al. 2011). In fact, after the first commercial product based on fungal laccase was launched in 1996 by Novozymes, several types of fungal laccases have been used in textile industries (Rodriguez-Couto 2012). However, most commercially used fungal laccases have a very narrow optimum pH range of 3.5–5.5 toward phenolic substrates, such as guaiacol (http://www.brenda-enzymes.org/), and they lose their activities at neutral or alkaline pH (Xu 1997), thus limiting their application in modern industries (Madzak et al. 2006). Our results showed that PIE5 can decolorize highly efficiently indigo dye under neutral and alkaline conditions (Fig. 4). Compared to other fungal laccases, PIE5 showed a higher decolorization rate, while the decolorization required less mediator and enzyme (Campos et al. 2001). Furthermore, our results also showed that PIE5 possessed a similar or higher indigo dye decolorization rate (working at pH 7.0–7.5) compared to the commercial T. villosa laccase from Novozymes (working at optimum pH 5.0) (Table 2). Fungal laccases with high activity and stability at neutral and alkaline pHs are highly desirable for textile industries, because the commonly used acidic reaction conditions of fungal laccases in textile industries for deinking and bleaching require subsequent neutralization steps after application, which in turn results in high amounts of salts and leads to disposal and pollution problems. As increasing environmental considerations are concerned, eco-friendly processes are attracting more and more public attention. In addition, in textile staining, indigo dye usually shows better solvation at neutral and alkaline pH and causes less background staining of the jeans compared with the practice conducted in acidic conditions. Deinking by laccases at alkaline or neutral pH provides therefore products with higher added-values. Decolorization of indigo dye at neutral pH means a reduction in the use of neutralization chemicals and also less back-staining of the textiles by the indigo dye (Colomera and Kuilderd 2015). In conclusion, our results proved that the newly developed laccase variant PIE5 with an alkaline optimum pH and a better decolorization percentage for indigo dye has a good potential in such types of industrial applications.
Availability of data and materials
Baldrian P (2006) Fungal laccases-occurrence and properties. FEMS Microbiol Rev 30:215–242. https://doi.org/10.1111/j.1574-4976.2005.00010.x
Bertrand T, Jolivalt C, Briozzo P, Caminade E, Joly N, Madzak C, Mougin C (2002) Crystal structure of a four-copper laccase complexed with an arylamine: insights into substrate recognition and correlation with kinetics. Biochemistry 41:7325–7333. https://doi.org/10.1021/bi0201318
Bloom JD, Arnold FH (2009) In the light of directed evolution: pathways of adaptive protein evolution. Proc Natl Acad Sci 106:9995–10000. https://doi.org/10.1073/pnas.0901522106
Campos R, Kandelbauer A, Robra KH, Cavaco-paulo A, Gu GM (2001) Indigo degradation with purified laccases from Trametes hirsuta and Sclerotium rolfsii. J Biotechnol 89:131–139. https://doi.org/10.1016/S0168-1656(01)00303-0
Chauhan PS, Goradia B, Saxena A (2017) Bacterial laccase: recent update on production, properties and industrial applications. 3 Biotech 7:1–20. https://doi.org/10.1007/s13205-017-0955-7
Colomera A, Kuilderd H (2015) Biotechnological washing of denim jeans. Elsevier Ltd, Hoboken
Cusano AM, Mekmouche Y, Meglecz E, Tron T (2009) Plasticity of laccase generated by homeologous recombination in yeast. FEBS J 276:5471–5480. https://doi.org/10.1111/j.1742-4658.2009.07231.x
De La Torre M, Martín-Sampedro R, Fillat Ú, Eugenio ME, Blánquez A, Hernández M, Arias ME, Ibarra D (2017) Comparison of the efficiency of bacterial and fungal laccases in delignification and detoxification of steam-pretreated lignocellulosic biomass for bioethanol production. J Ind Microbiol Biotechnol 44:1561–1573. https://doi.org/10.1007/s10295-017-1977-1
Endo K, Tsujino Y, Tamiya E, Saito KO, Ikeda R, Takagi M (2012) Isolation of a novel alkaline-induced laccase from Flammulina velutipes and its application for hair coloring. J Biosci Bioeng 113:575–579. https://doi.org/10.1016/j.jbiosc.2012.01.001
Fang Z, Li T, Wang Q, Zhang X, Peng H, Fang W, Hong Y, Ge H, Xiao Y (2011) A bacterial laccase from marine microbial metagenome exhibiting chloride tolerance and dye decolorization ability. Appl Microbiol Biotechnol 89:1103–1110. https://doi.org/10.1007/s00253-010-2934-3
Fang Z, Zhou P, Chang F, Yin Q, Fang W, Yuan J, Zhang X, Xiao Y (2014) Structure-based rational design to enhance the solubility and thermostability of a bacterial laccase Lac15. PLoS ONE 9:e102423. https://doi.org/10.1371/journal.pone.0102423
Fang Z, Liu X, Chen L, Shen Y, Zhang X, Fang W, Wang X, Bao X, Xiao Y (2015) Identification of a laccase Glac15 from Ganoderma lucidum 77002 and its application in bioethanol production David Wilson. Biotechnol Biofuels 8:2–13. https://doi.org/10.1186/s13068-015-0235-x
Froehner S, Eriksson K (1975) Properties of the glycoprotein laccase immobilized by two methods. Acta Chem Scand B 29:691–694
Hakulinen N, Rouvinen J (2015) Three-dimensional structures of laccases. Cell Mol Life Sci 72:857–868. https://doi.org/10.1007/s00018-014-1827-5
Herrera-Zúñiga LD, Millán-Pacheco C, Viniegra-González G, Villegas E, Arregui L, Rojo-Domínguez A (2019) Molecular dynamics on laccase from Trametes versicolor to examine thermal stability induced by salt bridges. Chem Phys 517:253–264. https://doi.org/10.1016/j.chemphys.2018.10.019
Hoegger PJ, Kilaru S, James TY, Thacker JR, Kües U (2006) Phylogenetic comparison and classification of laccase and related multicopper oxidase protein sequences. FEBS J 273:2308–2326
Hu J, Zhang Y, Xu Y, Sun Q, Liu J, Fang W, Xiao Y, Kües U, Fang Z (2019) Gongronella sp. w5 elevates Coprinopsis cinerea laccase production by carbon source syntrophism and secondary metabolite induction. Appl Microbiol Biotechnol 103:411–425. https://doi.org/10.1007/s00253-018-9469-4
Jimenez-Juarez N, Baeza A, Roman-Miranda R, Vazquez-Duhalt R, Valderrama B, Sánchez-Amat A (2005) Alkali and halide-resistant catalysis by the multipotent oxidase from Marinomonas mediterranea. J Biotechnol 117:73–82. https://doi.org/10.1016/j.jbiotec.2005.01.002
Jones SM, Solomon EI (2015) Electron transfer and reaction mechanism of laccases. Cell Mol Life Sci 72:869–883. https://doi.org/10.1007/s00018-014-1826-6
Kües U, Rühl M (2011) Multiple multi-copper oxidase gene families in basidiomycetes-what for? Curr Genomics 12:72–94. https://doi.org/10.2174/138920211795564377
Li W, Zhao Y (2018) Salt tolerance of T. versicolor laccase: bioinformatics study and internal transportation of chloride, dioxygen, and water. Chem J Chin Univ 39:255–262
Madzak C, Mimmi MC, Caminade E, Brault A, Baumberger S, Briozzo P, Mougin C, Jolivalt C (2006) Shifting the optimal pH of activity for a laccase from the fungus Trametes versicolor by structure-based mutagenesis. Protein Eng Des Sel 19:77–84. https://doi.org/10.1093/protein/gzj004
Maestre-Reyna M, Liu WC, Jeng WY, Lee CC, Hsu CA, Wen TN, Wang AHJ, Shyur LF (2015) Structural and functional roles of glycosylation in fungal laccase from Lentinus sp. PLoS ONE 10:1–28. https://doi.org/10.1371/journal.pone.0120601
Magni C, Sessa F, Capraro J, Duranti M, Maf E (2018) Structural and functional insights into the basic globulin 7S of soybean seeds by using trypsin as a molecular probe. Biochem Biophys Res Commun 496:89–94. https://doi.org/10.1016/j.bbrc.2018.01.002
Mate DM, Alcalde M (2015) Laccase engineering: from rational design to directed evolution. Biotechnol Adv 33:25–40
Mate DM, Gonzalez-Perez D, Falk M, Kittl R, Pita M, De Lacey AL, Ludwig R, Shleev S, Alcalde M (2013a) Blood tolerant laccase by directed evolution. Chem Biol 20:223–231. https://doi.org/10.1016/j.chembiol.2013.01.001
Mate DM, Gonzalez-Perez D, Kittl R, Ludwig R, Alcalde M (2013b) Functional expression of a blood tolerant laccase in Pichia pastoris. BMC Biotechnol 13:1–12. https://doi.org/10.1186/1472-6750-13-38
Maté D, García-Burgos C, García-Ruiz E, Ballesteros AO, Camarero S, Alcalde M (2010) Laboratory evolution of high-redox potential laccases. Chem Biol 17:1030–1041. https://doi.org/10.1016/j.chembiol.2010.07.010
Mehra R, Meyer AS, Kepp KP (2018) Molecular dynamics derived life times of active substrate binding poses explain KM of laccase mutants. RSC Adv 8:36915–36926. https://doi.org/10.1039/c8ra07138a
Mishra A, Kumar S, Kumar Pandey A (2011) Laccase production and simultaneous decolorization of synthetic dyes in unique inexpensive medium by new isolates of white rot fungus. Int Biodeterioration Biodegrad 65:487–493. https://doi.org/10.1016/j.ibiod.2011.01.011
Muñoz EM, Insuasti JP, Trujillo SD, Del Río A, Arroyave CS, Carrera MP, Soto AP, Pinchao JH (2017) Technology for denim finishing using laccase enzymes: a review. IOSR J Polym Text Eng 3:15–19. https://doi.org/10.9790/019X-03061519
Novoa C, Dhoke GV, Mate DM, Martínez R, Haarmann T, Schreiter M, Eidner J, Schwerdtfeger R, Lorenz P, Davari MD, Jakob F, Schwaneberg U (2019) KnowVolution of a fungal laccase toward alkaline pH. ChemBioChem. https://doi.org/10.1002/cbic.201800807
Paice MG, Bourbonnais R (1990) Oxidation an expanded of non-phenolic substrates role for lactase in lignin biodegradation. FEBS Lett 267:99–102. https://doi.org/10.1016/0014-5793(90)80298-W
Pan K, Zhao N, Yin Q, Zhang T, Xu X, Fang W, Hong Y, Fang Z, Xiao Y (2014) Induction of a laccase Lcc9 from Coprinopsis cinerea by fungal coculture and its application on indigo dye decolorization. Bioresour Technol 162:45–52. https://doi.org/10.1016/j.biortech.2014.03.116
Pardo I, Santiago G, Gentili P, Lucas F, Monza E, Medrano FJ, Galli C, Martínez AT, Guallar V, Camarero S (2016) Re-designing the substrate binding pocket of laccase for enhanced oxidation of sinapic acid. Catal Sci Technol 6:3900–3910. https://doi.org/10.1039/c5cy01725d
Pezzella C, Guarino L, Piscitelli A (2015) How to enjoy laccases. Cell Mol Life Sci 72:923–940. https://doi.org/10.1007/s00018-014-1823-9
Piontek K, Antorini M, Choinowski T (2002) Crystal structure of a laccase from the fungus Trametes versicolor at 1.90-A resolution containing a full complement of coppers. J Biol Chem 277:37663–37669
Rodgers CJ, Blanford CF, Giddens SR, Skamnioti P, Armstrong FA, Gurr SJ (2010) Designer laccases: a vogue for high-potential fungal enzymes? Trends Biotechnol 28:63–72. https://doi.org/10.1016/j.tibtech.2009.11.001
Rodriguez-Couto S (2012) Laccases for denim bleaching: an eco-friendly alternative. Open Text J 5:1–7. https://doi.org/10.2174/1876520301205010001
Rühl M, Majcherczyk A, Kües U (2013) Lcc1 and Lcc5 are the main laccases secreted in liquid cultures of Coprinopsis cinerea strains. Antonie van Leeuwenhoek Int J Gen Mol Microbiol 103:1029–1039. https://doi.org/10.1007/s10482-013-9883-7
Ruijssenaars HJ, Hartmans S (2004) A cloned Bacillus halodurans multicopper oxidase exhibiting alkaline laccase activity. Appl Microbiol Biotechnol 65:177–182. https://doi.org/10.1007/s00253-004-1571-0
Scheiblbrandner S, Breslmayr E, Csarman F, Paukner R, Führer J, Herzog PL, Shleev SV, Osipov EM, Tikhonova TV, Popov VO, Haltrich D, Ludwig R, Kittl R (2017) Evolving stability and pH-dependent activity of the high redox potential Botrytis aclada laccase for enzymatic fuel cells. Sci Rep 7:1–13. https://doi.org/10.1038/s41598-017-13734-0
Schwaneberg U, Zhang L, Cui H, Zou Z, Mirzaeigarakani T, Novoa-Henriquez C, Jooyeh B (2018) Directed evolution of a bacterial laccase (CueO) for enzymatic biofuel cells. Angew Chemie Int Ed. https://doi.org/10.1002/anie.201814069
Shigeno M, Kushida Y, Yamaguchi M (2015) Self-catalysis in thermal hysteresis during random-coil to helix-dimer transition of the sulfonamidohelicene tetramer. Chem Commun 51:4040–4043. https://doi.org/10.1039/c4cc10418h
Sitarz AK, Mikkelsen JD, Meyer AS (2016) Structure, functionality and tuning up of laccases for lignocellulose and other industrial applications. Crit Rev Biotechnol 36:70–86. https://doi.org/10.3109/07388551.2014.949617
Stajich JE, Wilke SK, Ahren D, Au CH, Birren BW, Borodovsky M, Burns C, Canback B, Casselton LA, Cheng CK, Deng J, Dietrich FS, Fargo DC, Farman ML, Gathman AC, Goldberg J, Guigo R, Hoegger PJ, Hooker JB, Huggins A, James TY, Kamada T, Kilaru S, Kodira C, Kües U, Kupfer D, Kwan HS, Lomsadze A, Li W, Lilly WW, Ma L-J, Mackey AJ, Manning G, Martin F, Muraguchi H, Natvig DO, Palmerini H, Ramesh MA, Rehmeyer CJ, Roe BA, Shenoy N, Stanke M, Ter-Hovhannisyan V, Tunlid A, Velagapudi R, Vision TJ, Zeng Q, Zolan ME, Pukkila PJ (2010) Insights into evolution of multicellular fungi from the assembled chromosomes of the mushroom Coprinopsis cinerea (Coprinus cinereus). Proc Natl Acad Sci 107:11889–11894. https://doi.org/10.1073/pnas.1003391107
Torres-Salas P, Mate DM, Ghazi I, Plou FJ, Ballesteros AO, Alcalde M (2013) Widening the pH activity profile of a fungal laccase by directed evolution. ChemBioChem 14:934–937. https://doi.org/10.1002/cbic.201300102
Xu F (1997) Effects of redox potential and hydroxide inhibition on the pH activity profile of fungal laccases. J Biol Chem 272:924–928. https://doi.org/10.1074/jbc.272.2.924
Xu F, Berka RM, Wahleithner JA, Nelson BA, Shuster JR, Brown SH, Palmer AE, Solomon EI (1998) Site-directed mutations in fungal laccase: effect on redox potential, activity and pH profile. Biochem J 334:63–70. https://doi.org/10.1042/bj3340063
Xu G, Wang J, Yin Q, Fang W, Xiao Y, Fang Z (2019) Expression of a thermo- and alkali-philic fungal laccase in Pichia pastoris and its application. Protein Expr Purif 154:16–24. https://doi.org/10.1016/j.pep.2018.09.015
This work was supported by the Natural Science Foundation of China (Grant number 31300044, 31600078) and the Open Fund for Discipline Construction, Institute of Physical Science and Information Technology (S030162001/016), and Doctoral Research Start-up Funding of Anhui University (Y040418162, Y040438001).
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The authors declare that they have no competing interests.
Primers used in this study. Fig. S1. Sequence alignment of Lcc9 and laccase sequences from other basidiomycetes. ▲ indicates the mutated amino acids. Fig. S2. Stereo views of the three types of cupper binding sites in C. cinerea Lcc9 and the mutated sites in variant PIE5. The copper atoms, one type-1 (T1), one type-2 (T2), and, two type-3 (T3a and T3b), are coordinated by the surrounding ten conserved histidines, one conserved cysteine and two water molecules. Protein residues are shown as a link model, the oxygen atoms are shown in red, nitrogen in blue, sulfur in yellow, and carbon in green. The four copper ions and water (Wat1 and Wat2) molecules are represented by blue and red spheres, respectively. a, rLcc9; b, PIE5. Fig. S3. Native PAGE analysis of the purified rLcc9, PIE5, and the specific mutants. Proteins were stained with 1 mM guaiacol in citrate/phosphate buffer (pH 4.0).
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Yin, Q., Zhou, G., Peng, C. et al. The first fungal laccase with an alkaline pH optimum obtained by directed evolution and its application in indigo dye decolorization. AMB Expr 9, 151 (2019). https://doi.org/10.1186/s13568-019-0878-2
- Fungal laccase
- Directed evolution
- Alkaline pH activity
- Indigo dye