Methicillin-resistant Staphylococcus aureus (MRSA) is one of the most threatening pathogens due to its multi-drug resistance (MDR) and strong biofilm-forming capacity. Here, we described the screening of a novel chimeolysin (ClyF) that was active against planktonic and biofilm MRSA. Biochemical tests showed that ClyF was active against all S. aureus clinical isolates tested under planktonic and biofilm conditions. Structure analysis revealed that ClyF has an enhanced thermostability and pH tolerance than its parental lysin Pc by forming a hydrophobic cleft in the catalytic domain and an Ig-like structure in the cell-wall binding domain. A single intraperitoneally or topically administration of ClyF showed good MRSA removing efficacy in mouse models of bacteremia and burn wound infection, respectively. Our data collectively demonstrated that ClyF has good bactericidal activity against planktonic and biofilm MRSA both in vitro and in vivo, and therefore represents a useful antibacterial to combat MDR S. aureus.
Staphylococcus aureus is an opportunistic pathogen that commonly colonizes nasopharynx and skin1, however, most of these strains have the capacity to cause severe infections when getting access to wounds and soft tissues, even progress to life-threatening diseases such as pneumonia or necrotizing fasciitis2. Due to its strong biofilm formation capacity and extensive antimicrobial resistance3, methicillin-resistant S. aureus (MRSA) biofilm-associated infections are more difficult to treat with antibiotics4. This is significant because S. aureus cells within biofilms can be a hundred to thousands of times more tolerant to common antibiotics5. MRSA biofilms are thus an important contributing factor for many treatment failures6, persistent infections7, increased risk of replacement of medical devices8, and the morbidity and mortality of most MRSA associated infectious diseases9.
Lysins are phage encoded cell-wall hydrolases that cleave the bacterial peptidoglycan for the release of progeny virions10. Because of their potent species-specific activities and rare bacterial resistance reported, lysins have received particular attention as promising alternatives to antibiotics11,12,13. In the last decade, several staphylococci targeted lysins have been developed and examined in experimental animal models to validate their efficacy as therapeutic agents14. However, natural staphylococcal lysins frequently suffer from solubility/stability and activity problems15,16. Moreover, the activities of some staphylococcal lysins are evidenced to be affected by working conditions, such as milk17, and ions concentrations18.
Natural lysins from phages infecting Gram-positive bacteria have a modular structure, that is, an N-terminal catalytic domain (CD) and a C-terminal cell-wall binding domain (CBD). Developing chimeric lysins (chimeolysins) by shuffling these two domains from different natural lysins has been demonstrated to be a promising strategy for developing novel antibacterials with improved properties12, such as enhanced activity19, improved solubility16, extended host range20, and intracellular killing capacity21. However, the current trial-and-error approach for identifying ideal chimeolysins is inefficient, making new strategies imperative. Our previous study has described an induced lysis-based screening method and its application in rapid screening of chimeolysins against streptococci22. This method is based on finding active bactericidal chimeolysins from a chimeolysin library with different combinations of CDs and CBDs expressed in E. coli by checking clear zones on culture plates. The chimeolysins inside E. coli cells were released by the aid of a novel enzyme, ClyN, which can cause controlled lysis of E. coli cells.
In the present study, a novel staphylolytic chimeolysin, ClyF, was identified using the screening method, and its bactericidal activity against planktonic and biofilm MRSA was further ascertained in vitro and in vivo in mouse models of bacteremia and burn wound infection.
Screening of chimeolysins against staphylococci
To identify chimeolysins active against S. aureus, a library of 126 chimeolysin clones representing chimeras of a random combination of the seven CDs and the three CBDs were screened for the ability to form large, clear lysis zones in a lawn of S. aureus N315. One clone, AK114, was distinguished by the production of the largest clear zone in the lawn of the target bacterium (Supplementary Fig. S1). Sequencing analysis showed that the chimeolysin produced by the clone AK114 is consisted of the CD from the Ply187 lysin (Pc, the N-terminal 157 amino acids) and the CBD from the PlySs2 lysin (PlySb, the C-terminal 99 amino acids), and this chimeolysin is named as ClyF for short. Because ClyF showed the highest activity on plates, its characteristics were further studied.
Characteristics of ClyF
Initially, we tested the chemical and enzymatic characteristics of ClyF. ClyF was expressed by E. coli as a soluble protein after induced overnight at 16 °C (Supplementary Fig. S2A), and after purification by Ni-NTA affinity chromatography a purity of >95% was obtained as shown by 12% SDS-PAGE gel (Supplementary Fig. S2B). As shown in Fig. 1A, ClyF was highly active against S. aureus, decreasing the turbidity of S. aureus N315 from 1.0 to near 0.1 within 5 min after treatment with 25 μg/ml ClyF, and leading to a reduction of 3.1 log10 in viable cell number.
Next, we tested the effects of temperature, pH, EDTA and NaCl on the lytic activity of ClyF in order to understand the working conditions of ClyF. Results showed that ClyF maintained over 85% activity after 1 h exposure to 55 °C and totally lost its activity after 1 h at 65 °C (Fig. 1B). The comparison tests of ClyF activity in buffers with different pHs showed that the pH tolerance range for ClyF was 4–10 (with a maximal activity at pH 6) (Fig. 1C), broader than that of Pc (which shows a pH range of 4–7, Supplementary Fig. S3). Further tests showed that EDTA (left-Y in Fig. 1D) and NaCl (right-Y in Fig. 1D) influenced the lytic activity of ClyF in a dose-dependent manner. Furthermore, we tested the storage stability of ClyF in various conditions. Our results showed that ClyF maintains 91.8%, 85.5% and 98.4% activity after being stored at room temperature (RT) for 1 month (Fig. 1E), 4 °C for 4 months (Fig. 1F), and −80 °C for 10 months (Fig. 1G), respectively. Notably, the lytic activity of ClyF was decreased drastically over the time period when stored at RT, nearly abolished after being stored for 4 months (Fig. 1E).
Secondary structure of ClyF
In order to assess whether PlySb enhanced the conformational stability of ClyF, we compared the secondary structures and melting temperature (Tm) of ClyF and Pc. As shown in Fig. 1H, the circular dichroism spectrum of ClyF looks smoother in lineshape compared to its parental lysin Pc. The secondary structure evaluation results indicated that the α-helix content of ClyF decreases slightly (8.2% in ClyF vs 17.7% in Pc), and the antiparallel content increases largely (46.5% in ClyF vs 22.3% in Pc) (Supplementary Table S3), corresponding to the fusion of PlySb. The thermal stability of ClyF and Pc was then assessed by following changes in the circular dichroism spectra in response to increasing temperature (Fig. 1I). Results showed that the Tm of ClyF and Pc was 65.03 ± 0.28 °C and 55.73 ± 0.18 °C, respectively, suggesting that the PlySb binding domain enhances the thermal stability of ClyF.
3D structural analysis of ClyF
The BLAST results showed that Pc was the member of NLPC_P60 superfamily and the CBD of ClyF belongs to the member of SH3 superfamily. To understand the structure difference between Pc and ClyF, we performed molecular modelling in silico. The secondary structure comparison performed with Dali server indicated that Pc/ClyF structures were similar to lysin LysK from S. aureus bacteriophage K. The 3D models of Pc/ClyF were constructed by Rosetta3.523 to further investigate how the CBD improved the Tm and pH tolerance of ClyF. These models fitted very well and provided us putative detailed interactions between the CD and the CBD.
The structure of Pc revealed a papain-like topology with a hydrophobic cleft, where the catalytic triad is located and act on peptidoglycan substrate (Fig. 2A). The structure of ClyF contains both the CD and the CBD showed in an Ig-like structure (Fig. 2B). In ClyF, the occupancy of α-helices and strands is higher than Pc (Fig. 2C). Moreover, on the surface of the CBD there are almost hydrophilic residues, such as Glu, Asp, Lys, Arg, and His (Fig. 2C).
By comparing Pc structure with other proteins with a similar function and structure (endolysins, CHAP domains and others) by sequences alignment and superposition, we found that the catalytic residues are highly conserved (Supplementary Figure S4). In lysin LysGH15 (PDB ID: 4OLK)24 and LysK (PDB ID: 4CSH)25, the catalytic residues are Cys54, His117 and Glu134, while in the streptococcal phage lysin PlyC (PDB ID:4F88) the catalytic residues are Cys333 and His42026. The superposition found that the catalytic residues of Pc corresponds to Cys36, His99 and Asp116 (Fig. 2D, and Supplementary Figure S4B). These hypothetical catalytic residues are close to the hydrophobic cleft, which supports the possibility that the catalytic part of the molecule is located in the hydrophobic groove.
Lytic spectrum of ClyF
The susceptibility tests showed that ClyF was active against all staphylococcal isolates tested in PBS, including S. aureus, S. saprophyticus, S. equorum, S. sciuri, S. chromogenes, S. haemolyticus, S. epidermidis, S. capitis, and S. albus, but not other species tested (Fig. 3). Intra-species differences in initial rate of lysis were observed with the maximum rate of 211 ± 19.8 −mOD600nm/min versus the minimal rate of 71.7 ± 4.0 −mOD600nm/min in S. aureus. Similarly, a 7-fold difference was observed for two S. equorum isolates (29.6 ± 3.2 vs 210.9 ± 0.6 −mOD600nm/min for WHS11093 and WHS11085, respectively) and for two S. chromogenes isolates (21.5 ± 2.0 vs 197.2 ± 9.2 −mOD600nm/min for WHS11071 and WHS11077, respectively). However, the ultimate lysis outcomes in OD600nm were close between these two S. equorum isolates (Supplementary Fig. S5). The observed difference in lytic rate may be due to the strain-to-strain variation of these clinical isolates, a phenomenon that was also observed by others16,27,28.
Comparison of ClyF activity with other lysins
Four additional chimeolysins, namely Clys103 (chimeolysin purified from clone AK103), Clys105 (chimeolysin purified from clone AK105), Clys210 (chimeolysin purified from clone AK210) and Clys308 (chimeolysin purified from clone AK308), were discovered on the screening plates (Supplementary Fig. S2C). Their antibacterial activities against S. aureus N315 were further examined in comparison with ClyF. Results showed that the activity of Clys114 (ClyF) against S. aureus N315 was much higher (10–87 folds faster) than that of these four chimeolysins, quite consistent with the observations on the screening plates (Fig. 4A). Next, we examined the activity of ClyF in comparison with one of its parental lysin PlySs2 (Supplementary Fig. S2D) in PBS buffer. Results showed that the lytic profile of ClyF against S. aureus N315 was quite different from that of PlySs2, ClyF caused a rapid decrease in turbidity, while a lag phase (about 15 min) occurred for PlySs2 although the final outcome of its lysis was close to that of ClyF (Fig. 4B). The tests against five other clinical S. aureus isolates further validated the improved lytic rate of ClyF, 2.0–8.5 folds faster than that of PlySs2 (Fig. 4C). Although Pc alone shows high staphylolytic activity in buffer19, we suspected that the PlySb CBD could enhance the staphylococcal-targeting ability of ClyF in bio-matrix conditions. To test this hypothesis, we compared the activities of ClyF and Pc in several conditions, including PBS buffer, pasteurized milk, mouse serum, and fresh pigskin surface. Results showed that there was no obvious difference in bacteriolytic activity between ClyF and Pc in PBS buffer (Fig. 4C). However, ClyF displayed a much higher bactericidal activity than Pc in milk, serum (Fig. 4D), and on pigskin (Supplementary Fig. S6). In addition, we also noted that the chimera ClyF showed a significantly (p < 0.01) higher activity than Pc under pH 8 to 10 (Supplementary Fig. S3).
Biofilm removing efficacy of ClyF
The degradation efficiency of ClyF against established biofilms formed by various staphylococcal isolates were evaluated. The CV staining assay showed that all staphylococcal isolates tested could form biofilms and all biofilms showed good susceptibility to ClyF (Fig. 5). Indeed, significant decreases in biofilm mass from 25.2% (i.e. OD595nm from 3.367 ± 0.122 to 2.519 ± 0.134 for S. aureus WHS11091) to 93.5% (i.e. OD595nm from 2.542 ± 0.272 to 0.166 ± 0.039 for S. equorum WHS11085) were observed after ClyF treatment (Fig. 5).
Efficacy of ClyF in a systemic infection model of MRSA bacteremia
The in vivo antibacterial activity of ClyF was evaluated in a mouse model of MRSA bacteremia. As shown in Fig. 6, 100% of the mice challenged with 6 × 107 CFU WHS11081/mouse and treated with PBS died within 24 h, while a dose-dependent rescue was observed in mice treated with ClyF. Indeed, 20% (1/6), 50% (3/6) and 100% (6/6) survival rates were observed in mice treated with 25, 37.5 and 50 mg/kg ClyF, respectively. Statistical analysis showed that the survival rates in groups treated with 37.5 and 50 mg/kg ClyF have significant differences (P < 0.05) in comparison with that of PBS treated controls (Fig. 6A). Further tests showed that no mice died after exposure to ClyF, either in a single intraperitoneal administration of a high dose (100 mg/kg, n = 3, Fig. 6A) or repeated intraperitoneal administration of a low dose (25 mg/kg/day for five continuous days, n = 3, data not shown). The antibody protection assay demonstrated that repeated injection of ClyF could induce immune responses in mice (Fig. 6B). However, the immunized serum showed no obvious neutralization effect on the lytic activity of ClyF in vitro (Fig. 6C).
Efficacy of ClyF in a mouse model of burn wound infection
The biofilm degradation efficiency of ClyF against staphylococci in vivo was evaluated in a mouse model of burn wound infected by MRSA WHS11081 (1 × 107 CFU/mouse). As shown in Fig. 7A, the average bioburden on burn wound skin surface was increased to 9.2 × 108 cfu/g tissue (about 7.97 × 107 cfu/mouse) in the untreated group. While the average bioburden was increased to 1.6 × 109 cfu/g tissue (about 2.13 × 108 cfu/mouse) in PBS treated group, and in groups treated with 0.1 mg ClyF in a single dose or twice (ClyF*), the average bioburden was reduced to 4.6 × 107 cfu/g tissue (a reduction of 1.5 log10, about 5.34 × 106 cfu/mouse) and 7.7 × 105 cfu/g tissue (a reduction of 3.3 log10, about 8.47 × 104 cfu/mouse), respectively. The histological analysis showed that dense S. aureus community (purple-blue) existed below the epidermis of the skin in the untreated and the PBS treated groups, while less S. aureus clump was observed in the ClyF treated group (Fig. 7B, top row). Moreover, obvious fibrous matrix material could be seen beneath the S. aureus biofilm tissues (green arrows), and the accumulation of immune cells was observed under the fibrous layer in all treatment groups (Supplementary Fig. S7). The Gram staining analysis also showed heavy S. aureus clump in the untreated and the PBS treated groups (blank arrows), and reduced clusters of S. aureus at the wound surface in the ClyF treated group (Fig. 7B, bottom row, blue).
SEM was performed to further characterize the development of S. aureus biofilms. As shown in Fig. 7C, the wound skin surfaces in the untreated and the PBS treated groups were covered by dense and thick biofilms, including distinct matrix fibers and amorphous encasing material. While, in the group treated with ClyF in a single dose or twice doses, the biofilms were observed to be degraded and destroyed in the wounds (Supplementary Fig. S8). These results were consistent with the observations in the section staining analysis.
The increased emergency of MDR pathogens worldwide awakens some old therapeutics (i.e. phage therapy29) and also, evokes lots of new strategies. One promising alternative among these new strategies is the lysin-derived therapy developed in the latest 15 years. Several key advantages of lysins include: 1) just killing a designated special or closely related species, without disturbing normal microbial flora; 2) robust killing efficacy against both planktonic and biofilm bacteria without evoking detectable resistance. Although there are no lysin-derived drugs on the market yet, the recent progresses in clinical trials for two staphylococcal lysins (i.e. CF-30130 and P12831) suggest bright potential for treating bacterial infections by lysins.
In the present study, we described the rapid screening of chimeolysins against staphylococci by using the induced lysis-based screening method. The key features of the screening method contain: 1) a novel chimeric enzyme, ClyN, that induces the autolysis of the host E. coli cells from within upon induction with IPTG; and 2) an E. coli expression library constructed by random shuffling of CDs and CBDs from different lysins under the control of another promoter (i.e. PBAD). Transferring plasmid pET-clyN into the expression library allows us to find the clones that expressing active bactericidal chimeolysins directly on the lawn of a target strain. By using of this screening method one chimeolysin, ClyF, was found to show the clearest zone on the S. aureus N315 plates. Further expression-based activity tests confirmed that ClyF has a much higher antibacterial activity than other lysins sharing the same CBD (Fig. 4A). These results demonstrated that the screening method is indeed a useful tool for rapid identification of active chimeolysins.
Sequencing analysis showed that ClyF consists of the CBD domain from lysin PlySs2 (PlySb) and the catalytic domain from lysin Ply187 (Pc). PlySs2, also referred to as CF-301, is a unique lysin derived from S. suis phage that shows high lytic activity against streptococci and staphylococci28. Our previous study showed that the CD of PlySs2 alone only has a very weak lytic activity, and the CBD of PlySs2 (PlySb) has high affinities for streptococci32 and some staphylococci (unpublished data), indicating that the broad binding ability of PlySb contributes significantly to the broad lytic spectrum of PlySs2. However, the host range of ClyF is found to be restricted to staphylococci (Fig. 3). This may be due to the hydrolase specificity of its CD donor Pc, which is derived from a staphylococci-targeted lysin. But as shown in the secondary (Fig. 1H and Table S3) and 3D structure (Fig. 2) analysis of ClyF, PlySb domain could endow the new chimera ClyF some new characteristics. First, the antiparallel-rich PlySb domain could enhance the flexibility of ClyF under thermal and different pH conditions. As revealed by the circular dichroism denaturation test and the pH-dependent lytic activity assay, the Tm of ClyF increases 9.3 °C (Fig. 1I) and the pH tolerance of ClyF is extended to pH 8–10 (Supplementary Fig. S3) compared to that of Pc. Second, the 3D structure modeling of Pc and ClyF showed that the PlySb domain contains many hydrophilic and charged residues (Fig. 2C), which could contribute also to improve the pH tolerance of ClyF in extreme acidic (pH 2–4) or alkaline (pH 8–10) environments.
The superposition analysis revealed that the catalytic residues of Pc is probably Cys36, His99 and Asp116 (Fig. 2D, and Supplementary Fig. S4B), which may be critical for its peptidoglycan hydrolase activity. The importance of Cys and His residues have been evidenced in some lysins that sharing a similar domain with Pc by site-directed mutation examination, for instance in PlyC26 and LysGH1524. The comparison analysis also showed that the Asp116 is not as highly conserved as Cys36 and His99 in Pc (Supplementary Figure S4A), however, Asp116 may be involved in the formation of a special catalytic triad in combination with the other two residues, similar as the catalytic triad formed in the mycobacteriophage lysin B33, the CHAP domain of the enzyme (PDB code 2K3A) from Staphylococcus saprophyticus34, and the S. aureus bacteriophage lysin LysK25. Although our analysis revealed some new insights into the catalytic mechanism of Pc, the quantified contribution of these residues still needs further study.
One outstanding property of ClyF distinguishing it from other lysins is its robust lytic activity both in buffer and bio-matrices (i.e. milk and serum). Reductions of 3.1 and 7 log10 in viable cell number were observed after treatment with 25 μg/ml ClyF in PBS for 5 min (Fig. 1A), and 40 μg/ml ClyF in milk for 1 h (Fig. 4D), respectively. Such a high lytic activity in milk was not observed for many other staphylococcal lysins. Considering the contaminations of staphylococci in cow mastitis and milk preservation, ClyF could also be exploited to prevent/remove staphylococci in milk conditions. Interestingly, an improved staphylolytic activity, killing > 7 logs after treatment with 20 μg/ml ClyF for 1 h (Fig. 4D), was observed in serum, suggesting that ClyF has good potential in controlling blood infections caused by S. aureus, for instance, bacteremia.
The in vivo studies also demonstrated that ClyF has good activities against S. aureus infections in mouse models. When applied systemically, ClyF showed a dose-dependent rescue efficacy in a mouse model of MRSA bacteremia (Fig. 6A). Although ClyF evoked the immune response, the antibodies seem not neutralizing the activity of ClyF, suggesting that either the anti-ClyF antibodies do not hinder the activity or they do not efficiently compete for the binding of ClyF to its substrate as explained by others14,16. When applying topically, ClyF showed good biofilm eradication efficacy against MRSA colonized in mice burn wounds (Fig. 7). Burn wounds infected with MRSA may progress into cellulitis and more serious invasive disease, e.g. septicaemia, in hospital35,36, and thus becomes a problem that difficult to deal with. Although applying ClyF once has showed significant reduction of the bacteria in the wound, dosing ClyF every 6 hours (twice) demonstrated much better antibacterial activity as shown in Fig. 7A. These results showed that repeated treatment may be needed when applying ClyF topically. However, the formulation and storing stability of ClyF still need further testing before clinical application.
Besides ClyF, several other chimeolysins against S. aureus have also been developed in recent years, including P12831, ClyS16, PRF-11937, Ply187AN-KSH3b38, ClyH19, and Lys170-8739. Each of them has been demonstrated effective against planktonic S. aureus in vitro, and in animal infection models. P128 has also showed good lytic activity against S. aureus in simulated nasal fluid31 and human blood40. Several chimeolysins also showed good degradation efficacy against S. aureus biofilms formed in microplates (i.e. ClyH and Ply187AN-KSH3b). However, as far as we know, ClyF is the first one that shows good bactericidal activity against both planktonic and biofilm S. aureus in vitro and in vivo, and all coagulase-negative staphylococci tested (Fig. 3), a property that has not been tested for other chimeolysins.
To summarize, we reported here a novel chimeolysin, ClyF, which was identified from the induced lysis-based screening method and showed robust bactericidal activity against planktonic and biofilm MRSA both in vitro and in vivo. Taking into account its good stability and high staphylolytic activity against all staphylococci species tested, ClyF could be a useful antimicrobial to combat MDR staphylococci.
All bacterial strains (Supplementary Table S1) used in this study were grown in trypticase soy broth (TSB) medium at 37 °C, except Escherichia coli that was cultured in Luria-Broth (LB) medium. A collection of clinical staphylococcal isolates with different antibiogram profiles were identified by PCR-DNA sequencing analysis combined with biochemistry test using a MicroStation system (Biolog, GEN III Omnilog Combo Plus System, USA). The PCR profiles of the SCCmec and enterotoxin gene types of these staphylococcal isolates were listed in Supplementary Figures S9 and S10, respectively.
On-plate bactericidal chimeolysin screening
Our previous study has reported the screening of streptococci-targeted chimeolysins from an E. coli expression library containing combinations of seven CDs (from lysins Ply187, Ply118, Ply511, PlyGBS, PlySs2, and PlyC) and three CBDs (from lysins PlySs2, PlyV12 and LysAB2)22. Ply187 is a staphylococci-targeted lysin coded by S. aureus phage 18741. Ply118 and Ply511 are Listeria phage derived lysins42. PlyGBS43, PlySs228 and PlyC44 are streptococcal phage derived lysins, and PlySs2 also shows an extended lytic activity against staphylococci. PlyV12 is an enterococcal phage lysin with effective kill activity against Enterococcus faecalis and E. faecium27. LysAB2 is an Acinetobacter baumannii phage lysin that shows extended antibacterial activity against S. aureus45. Because several domains were derived from staphylolytic lysins, the expression library was also tested against staphylococci. Briefly, individual clones from the E. coli expression library were inoculated into 1 ml fresh LB medium with 0.2% L-arabinose in 24-well plates. After overnight incubation at 37 °C and replica plating, wells were supplied with 0.5 mM isopropyl-β-D-thiogalactoside (IPTG, to initiate the expression of ClyN that can cause the lysis of host E. coli cell from within), and immediately, a 5 μl aliquot of these cultures was spotted on top of LB-agar (LA) plates overlaid with soft-agar containing S. aureus N315. Clear zones were checked at drop deposition sites. Finally, the corresponding clones which generated the clear zones were sequenced from the replica plates. The sequences of chimeolysins obtained were listed in the Supplementary Material.
Construction of expression plasmids
To obtain a higher expression level, chimeolysins from clones AK103 (Clys103), AK105 (Clys105), AK114 (Clys114, or ClyF), AK210 (Clys210) and AK308 (Clys308) were sub-cloned into pET28a(+) plasmid, using the following primers (Supplementary Table S2): Clys103-F/Clys103-R for Clys103, Clys105-F/ClyR-R for Clys105, ClyF-F/ClyR-R for ClyF, Clys210-F/ClyR-R for Clys210, Clys308-F/ClyR-R for Clys308. Each construct was transformed into E. coli BL21(DE3) through the heat-shock method46, selected on LB agar plates containing 50 μg/ml Kanamycin, and confirmed by sequencing.
Recombinant proteins were purified through Ni-NTA affinity chromatography as described previously with minor modifications47. Briefly, bacterial cells were induced with 0.2 mM IPTG overnight at 16 °C and collected for protein purification after sonication on ice. Purification was performed by washing and eluting with 60 and 250 mM imidazole, respectively. After dialyzed against PBS buffer (137 mM NaCl, 2.7 mM KCl, 4.3 mM Na2HPO4·H2O, 1.4 mM KH2PO4, pH 7.4), purified proteins were stored at −80 °C till use.
The parental lysins Pc (CD of the Ply187 lysin) and PlySs2 were purified through Ni-NTA affinity chromatography as described previously in our laboratory19,32, specifically, eluting with 265 mM and 400 mM imidazole, respectively, followed by dialyzing against PBS.
Lytic activity assay
The bacteriolytic activity was determined as previously described48, with minor modifications. Briefly, bacteria cells were cultured overnight, centrifuged, and resuspended in PBS (pH 7.4) to a final OD600nm of 0.8–1.0. After mixing 195 μl of bacterial suspension with 5 μl of lysin (final concentration of 25 μg/ml) in a 96-well plate (Perkin-Elmer, USA), the drop of OD600nm in each well was monitored immediately by a microplate reader (Synergy H1, BioTek, USA) at 37 °C for 60 min. The bacterial suspension was mixed with ClyF by using of a multi-channel pipette in order to reduce the time lapse before reading (less than 5 s). The rate of lysis was measured as the drop in milli-OD600nm per minute (−mOD600nm/min) in the first 3 min as described elsewhere43. Meanwhile, the decrease in viable cells corresponding to the loss of turbidity was also tested by plating the aliquots from the lytic assay at various time points (0, 2, 5, and 15 min) to TSB agar for counting of CFU. Ten-fold dilution was performed immediately (to decrease ClyF rapidly to very low concentrations that show minimum lytic activities) to avoid possible killing during plating. To determine the influence of NaCl, EDTA and pH on the lytic activity of ClyF, S. aureus N315 cells were suspended in phosphate buffer containing various concentrations of NaCl (ranging from 50 to 500 mM) or EDTA (ranging from 50 to 500 μM), or universal buffers with pH ranging from 2 to 12. The universal buffer was made by mixing equal parts of 20 mM boric acid and 20 mM phosphoric acid, followed by titration with sodium hydroxide as described before49. After adding 25 μg/ml ClyF to the bacterial suspensions, OD600nm drops were monitored by the microplate reader at 37 °C for 60 min. The relative activities of ClyF in different NaCl, EDTA, and pH buffers were calculated by deducting the background signal of PBS treated wells and normalized by comparison with the maximum activity of ClyF in these buffers. To evaluate the effect of temperature, ClyF was stored at different temperatures ranging from 4 to 100 °C for 60 min and then cooled to room temperature (RT) for 10 min (prior to use in the assay) to determine the residual enzymatic activity. To determine the storage stability of ClyF, ClyF was stored at RT, 4 °C or −80 °C for different time periods (0–10 months), and the remaining activity against S. aureus N315 was measured at 37 °C (the frozen solutions were equilibrated to RT by placing the tubes at RT for 30 min before the assay) following the protocol described above. All experiments have been repeated for at least three times (or at least three microplate wells for each repeat), using PBS treated wells as controls.
Compare the lytic activity of ClyF with other lysins
ClyF was further compared with four other chimeolysins discovered on the screening plates, namely Clys105, Clys210, Clys308, and Clys103 (Clys105, Clys210 and Clys308 were found to share the same CBD with ClyF, and Clys103 shares the same CD with PlySs2). A 5 μl aliquot of each protein (0.87 μM each) was mixed with 195 μl S. aureus N315 suspension followed by monitoring the decrease of OD600nm at 37 °C for 60 min. To compare the activity of ClyF with its parental lysin PlySs2, the lytic profiles of ClyF and PlySs2 (0.35 μM each) against six S. aureus isolates in PBS buffer were determined.
Compare the lytic activity of ClyF with Pc in bio-matrix conditions
In order to study the possible role of PlySb played in ClyF, we compared the lytic activity of ClyF with that of Pc under various bio-matrix conditions, including PBS buffer, milk, mouse serum and fresh pigskin surface. For testing the activity in milk and serum, staphylococcal isolates were resuspended in pasteurized milk and serum, respectively, and treated with different concentrations of ClyF or Pc (0, 0.7, or 1.4 μM) at 37 °C for 60 min. The number of residual viable cell after each treatment was determined by plating on LA plates. For testing the activity on pigskin, fresh pigskins (pre-cut into 2 × 2 cm2 square and treated with UV light for 30 min) were inoculated with 20 μl of S. aureus N315 cells (about 1 × 107 cfu) and incubated at 37 °C for 1 h. After 20 μl of 0.25 mg/ml ClyF or Pc was applied for various times (1–4 h), pigskin was cut up and vortexed vigorously in 0.5 ml PBS for 1 min, then the viable cell number was calculated by plating serial dilutions on Baird-Parker agar plates (selective culture for S. aureus). All the above experiments were performed in triplicate using PBS treated groups as controls.
Biofilm removing efficacy of ClyF
The efficiency of ClyF against established biofilms was determined by crystal violet (CV) staining50. Briefly, staphylococcal isolates, including S. aureus, Staphylococcus saprophyticus, Staphylococcus equorum, Staphylococcus sciuri, Staphylococcus chromogenes and Staphylococcus haemolyticus, were cultured in 96-well polystyrene plates (Tissue culture treated, Nest Biotech Co., China) supplied with TSBG (TSB with 1% glucose) medium for 24 h to develop biofilms. After washing twice with PBS, wells were treated either with 200 μl of 100 μg/ml ClyF, or an equal volume of PBS, at 37 °C for 45 min. After washing two times with PBS, wells were dried and stained with 200 μl of 0.1% CV (Merck, USA) at RT for 5 min. Following that, wells were washed two times with distilled water, solubilized with 200 μl ethanol and measured by a microplate reader at OD595nm as described elsewhere51. The final biofilm masses in ClyF treated wells were analyzed by one-way analyses of variance (ANOVA) in comparison with that of the PBS treated wells. Difference with p < 0.05 was considered statistically significant. All experiments have been repeated for at least three times (at least triplicate microplate wells for each repeat).
Immunological neutralization test
The neutralization effect of ClyF-specific antibodies on the activity of ClyF was tested as described previously16. Briefly, mice were injected with ClyF (0.5 mg) 3 times on 10-day intervals. Mice sera were sampled 15 days after the last injection, the titers of ClyF-specific antibody (>10,000) were determined by coating ClyF on a microplate and using horseradish peroxidase-conjugated goat anti-mouse IgG following the instructions of a commercial ELISA kit (QF-Bio, Shanghai, China). To determine the neutralization effect of immunized serum, ClyF (20 μg/ml in 90 μl volume) was pre-mixed with 10 μl of either ClyF immunized mouse serum (the final antibody titer was about 1:1,000), or preimmune serum, or PBS in a 96-well plate at 37 °C for 15 min. After adding an equal volume of S. aureus N315 bacterial suspension (100 μl to give a final ClyF concentration of 10 μg/ml), the decrease of OD600nm in wells treated with the immunized serum were measured by a microplate reader and compared to those of preimmune serum and PBS treated wells.
All mouse experiments were carried out in an ABSL-2 lab and all experimental methods were carried out in accordance with the regulations and guidelines set forth by the Animal Experiments Committee of Wuhan Institute of Virology, Chinese Academy of Sciences. All experimental protocols were approved by the Animal Experiments Committee of Wuhan Institute of Virology, Chinese Academy of Sciences (approval no. WIVA17201401). Animals were cared in individually ventilated cages following a set of animal welfare and ethical criteria during the experiences, and euthanized at the end of observation.
Systemic infection model of MRSA bacteremia
In the mouse systemic infection model, female BALB/c mice (SPF-level, 6–8 weeks old, obtained from Wuhan Institute of Biological Products Co., Ltd, Wuhan, China) were injected intraperitoneally with different concentrations of MRSA WHS11081 to determine the minimal lethal dose (MLD) that caused 100% mortality within one day. Then, mice were inoculated intraperitoneally with 2 × MLD of WHS11081 cells (6 × 107 CFU/mouse in 200 μl volume). Three hours after challenging, mice were divided into 4 groups randomly. Three groups (n = 6) received 25, 37.5 and 50 mg/kg ClyF intra-peritoneally (in a volume of 0.5 ml), respectively, and the fourth group (n = 5) was injected with PBS buffer (0.5 ml) only. To evaluate the toxicity of ClyF, non-infected mice received a single-dose of 100 mg/kg ClyF (n = 3), or 25 mg/kg per day for five continuous days (n = 3). The survival rates for all groups were recorded over 7 days. Survival data of ClyF treated groups were analyzed by one-way ANOVA in comparison with that of the PBS treated control.
Topical infection model of burn wound
In the burn wound skin model, 6–8 weeks old female BALB/c mice (SPF-level, and confirmed by plating on Baird Parker plates to exclude any natural staphylococcal flora on the mouse skin) were anesthetized by intraperitoneal injection of pentobarbital at 50 mg/kg and then shaved with an electric razor to create a 2-cm2 hairless area on dorsum as described52. Partial thickness burn was achieved by exposure of the naked skin to 80 °C water for 10 s. The burn was then inoculated with 1 × 107 CFU WHS11081 (in 5 μl TSB). At 24 h post-colonization, mice were randomly separated into four groups as following: group 1 was left untreated (n = 6); group 2 was treated with 50 μl PBS only (n = 6); group 3 received a single-dose of 0.1 mg ClyF topically in 50 μl PBS (n = 8) and group 4 received two doses of 0.1 mg ClyF topically in 50 μl PBS at 6 h intervals (n = 8). 24 h post-treatment, mice were sacrificed by cervical dislocation method for skin harvesting. Specifically, all the infected wound area was excised, weighed, and homogenized in 1 ml PBS for 30 s. The viable cell number in each tissue sample was calculated by plating tissue dilutions onto Baird-Parker agar plates and analyzed by one-way ANOVA. To test whether ClyF carryover could have occurred during dilution and plating procedures, residual enzymatic activity of ClyF on the skin surface was tested. Briefly, tissue samples were homogenized in PBS and centrifuged at 10,000 g for 1 min, then the supernatant (100 μl) was mixed with S. aureus N315 cells and the enzymatic activity was determined immediately by monitoring the changes in OD600nm, using PBS as control. No decrease in OD600nm was observed as monitored by the microplate reader, indicating that no active ClyF was remained after 24 h on the skin surface (data not shown).
Hematoxylin and eosin staining
After 24 h of treatment, skin tissues taken for histological analysis were fixed with formalin and embedded in paraffin. Sections (Thermo Cytospin 4) were either Gram stained or stained with hematoxylin and eosin (H&E) using an automatic immunohistochemical stainer (Autostainer 480&PT, Thermo Scientific, USA). Samples were imaged and analyzed by an automatic digital slide scanner (Pannoramic MIDI, 3DHISTCH, Hungary).
Scanning electron microscope
To visualize MRSA biofilms in burn wounds, skin tissues (treated with PBS or ClyF) were harvested, fixed with 2.5% glutaraldehyde and dehydrated by granted ethanol (from 30% to 100%). After treatment with critical point drying and sputter-coated with gold, tissue samples were examined by a scanning electron microscope (SEM, SU8010, Hitachi, Japan). Images were taken at ×20,000 magnification under the same instrument conditions.
The circular dichroism spectra were collected with an Applied Photophysics Chirascan plus circular dichroism spectrometer (Leatherhead, UK). For native structure measurement, spectra of ClyF (7.7 μM) and Pc (10.7 μM) in 4 mM Tris-HCl (pH 7.4) were recorded from 190–260 nm (0.1 cm path length) at RT. The spectra of air and buffer were recorded as background and baseline, respectively. For evaluation of thermal stability, the melting temperature (Tm) of ClyF (38.5 μM) and Pc (21.4 μM) in 4 mM Tris-HCl (pH 7.4) were measured at 220 nm by recording the circular dichroism signal at a temperature range of 25–90 °C. The secondary structures and Tms of ClyF and Pc were calculated by CDNN V2.1 software supplied by the instrument provider.
Construction of 3D models of Pc and ClyF
The 3D models of Pc and ClyF were constructed by Rosetta 3.523. Rosetta provided both ab initio and comparative models of protein domains using the Rosetta fragment insertion method. Domains without a detectable PDB homolog were modeled with the Rosetta de novo protocol. Comparative models were built from parent PDBs detected by PSI-BLAST or HHSEARCH and aligned by HHSEARCH and SPARKS. Loop regions were assembled from fragments and optimized to fit the aligned template structure53. The manual model building was performed with Coot54. And the quality of modeled 3D structures was checked using MolProbity55.
How to cite this article: Yang, H. et al. A novel chimeric lysin with robust antibacterial activity against planktonic and biofilm methicillin-resistant Staphylococcus aureus. Sci. Rep. 7, 40182; doi: 10.1038/srep40182 (2017).
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Chuang, Y. Y. & Huang, Y. C. Molecular epidemiology of community-associated meticillin-resistant Staphylococcus aureus in Asia. Lancet Infect. Dis. 13, 698–708, doi: 10.1016/S1473-3099(13)70136-1 (2013).
Holland, T. L., Arnold, C. & Fowler, V. G., Jr. Clinical management of Staphylococcus aureus bacteremia: a review. JAMA 312, 1330–1341, doi: 10.1001/jama.2014.9743 (2014).
Pasberg-Gauhl, C. A need for new generation antibiotics against MRSA resistant bacteria. Drug Disc . Today 11, 109–116, doi: 10.1016/j.ddtec.2014.04.001 (2014).
Otto, M. MRSA virulence and spread. Cell Microbiol. 14, 1513–1521, doi: 10.1111/j.1462-5822.2012.01832.x (2012).
Wu, J. A., Kusuma, C., Mond, J. J. & Kokai-Kun, J. F. Lysostaphin Disrupts Staphylococcus aureus and Staphylococcus epidermidis Biofilms on Artificial Surfaces. Antimicrob. Agents Chemother. 47, 3407–3414, doi: 10.1128/aac.47.11.3407-3414.2003 (2003).
Otto, M. Staphylococcal infections: mechanisms of biofilm maturation and detachment as critical determinants of pathogenicity. Ann. Rev. Med. 64, 175–188, doi: 10.1146/annurev-med-042711-140023 (2013).
Fauvart, M., De Groote, V. N. & Michiels, J. Role of persister cells in chronic infections: clinical relevance and perspectives on anti-persister therapies. J. Med. Microbiol. 60, 699–709, doi: 10.1099/jmm.0.030932-0 (2011).
Jones, S. M., Morgan, M., Humphrey, T. J. & Lappin-Scott, H. Effect of vancomycin and rifampicin on meticillin-resistant Staphylococcus aureus biofilms. Lancet 357, 40–41, doi: 10.1016/S0140-6736(00)03572-8 (2001).
Pollitt, E. J., Crusz, S. A. & Diggle, S. P. Staphylococcus aureus forms spreading dendrites that have characteristics of active motility. Sci. Rep. 5, 17698, doi: 10.1038/srep17698 (2015).
Szweda, P. et al. Peptidoglycan hydrolases-potential weapons against Staphylococcus aureus . Appl. Microbiol. Biotechnol. 96, 1157–1174, doi: 10.1007/s00253-012-4484-3 (2012).
Rodriguez-Rubio, L. et al. Phage lytic proteins: biotechnological applications beyond clinical antimicrobials. Crit. Rev. Biotechnol. 1–11, doi: 10.3109/07388551.2014.993587 (2015).
Yang, H., Yu, J. & Wei, H. Engineered bacteriophage lysins as novel anti-infectives. Front. Microbiol. 5, 542 (2014).
Pastagia, M., Schuch, R., Fischetti, V. A. & Huang, D. B. Lysins: the arrival of pathogen-directed anti-infectives. J. Med. Microbiol. 62, 1506–1516, doi: 10.1099/jmm.0.061028-0 (2013).
Fischetti, V. A. Lysin Therapy for Staphylococcus aureus and Other Bacterial Pathogens. Curr. Top. Microbiol. Immunol. 1–12, doi: 10.1007/82_2015_5005 (2016).
Resch, G., Moreillon, P. & Fischetti, V. A. A stable phage lysin (Cpl-1) dimer with increased antipneumococcal activity and decreased plasma clearance. Int. J. Antimicrob. Agents 38, 516–521, doi: 10.1016/j.ijantimicag.2011.08.009 (2011).
Daniel, A. et al. Synergism between a Novel Chimeric Lysin and Oxacillin Protects against Infection by Methicillin-Resistant Staphylococcus aureus . Antimicrob. Agents Chemothe 54, 1603–1612, doi: 10.1128/aac.01625-09 (2010).
Obeso, J. M., Martinez, B., Rodriguez, A. & Garcia, P. Lytic activity of the recombinant staphylococcal bacteriophage PhiH5 endolysin active against Staphylococcus aureus in milk. Int. J. Food Microbiol. 128, 212–218, doi: 10.1016/j.ijfoodmicro.2008.08.010 (2008).
Linden, S. B. et al. Biochemical and biophysical characterization of PlyGRCS, a bacteriophage endolysin active against methicillin-resistant Staphylococcus aureus . Appl. Microbiol. Biotechnol. 99, 741–752, doi: 10.1007/s00253-014-5930-1 (2015).
Yang, H. et al. Novel chimeric lysin with high-level antimicrobial activity against methicillin-resistant Staphylococcus aureus in vitro and in vivo . Antimicrob. Agents Chemother. 58, 536–542, doi: 10.1128/AAC.01793-13AAC.01793-13 (2014).
Dong, Q. et al. Construction of a chimeric lysin Ply187N-V12C with extended lytic activity against staphylococci and streptococci. Microbial. Biotechnol. 8, 210–220, doi: 10.1111/1751-7915.12166 (2015).
Becker, S. C. et al. Triple-acting Lytic Enzyme Treatment of Drug-Resistant and Intracellular Staphylococcus aureus . Sci. Rep. 6, 25063, doi: 10.1038/srep25063 (2016).
Yang, H. et al. A chimeolysin with extended-spectrum streptococcal host range found by an induced lysis-based rapid screening method. Sci. Rep. 5, 17257, doi: 10.1038/srep17257 (2015).
Leaver-Fay, A. et al. ROSETTA3: an object-oriented software suite for the simulation and design of macromolecules. Method. Enzymol. 487, 545–574, doi: 10.1016/B978-0-12-381270-4.00019-6 (2011).
Gu, J. et al. Structural and biochemical characterization reveals LysGH15 as an unprecedented “EF-hand-like” calcium-binding phage lysin. PLoS Pathog. 10, e1004109, doi: 10.1371/journal.ppat.1004109 (2014).
Sanz-Gaitero, M., Keary, R., Garcia-Doval, C., Coffey, A. & van Raaij, M. J. Crystal structure of the lytic CHAP(K) domain of the endolysin LysK from Staphylococcus aureus bacteriophage K. Virol. J. 11, 133, doi: 10.1186/1743-422X-11-133 (2014).
McGowan, S. et al. X-ray crystal structure of the streptococcal specific phage lysin PlyC. Proc. Natl. Acad. Sci. USA 109, 12752–12757, doi: 10.1073/pnas.1208424109 (2012).
Yoong, P., Schuch, R., Nelson, D. & Fischetti, V. A. Identification of a broadly active phage lytic enzyme with lethal activity against antibiotic-resistant Enterococcus faecalis and Enterococcus faecium . J. Bacteriol. 186, 4808–4812, doi: 10.1128/JB.186.14.4808-4812.2004186/14/4808 (2004).
Gilmer, D. B., Schmitz, J. E., Euler, C. W. & Fischetti, V. A. Novel bacteriophage lysin with broad lytic activity protects against mixed infection by Streptococcus pyogenes and methicillin-resistant Staphylococcus aureus . Antimicrob. Agents Chemother. 57, 2743–2750, doi: 10.1128/AAC.02526-12AAC.02526-12 (2013).
Young, R. & Gill, J. J. Phage therapy redux–What is to be done? Science 350, 1163–1164, doi: 10.1126/science.aad6791 (2015).
Schuch, R. et al. Combination therapy with lysin CF-301 and antibiotic is superior to antibiotic alone for treating methicillin-resistant Staphylococcus aureus-induced murine bacteremia. J. Infect. Dis. 209, 1469–1478, doi: 10.1093/infdis/jit637 (2014).
Vipra, A. A. et al. Antistaphylococcal activity of bacteriophage derived chimeric protein P128. BMC Microbiol. 12, 41, doi: 10.1186/1471-2180-12-411471-2180-12-41 (2012).
Huang, Y., Yang, H., Yu, J. & Wei, H. Molecular dissection of phage lysin PlySs2: integrity of the catalytic and cell wall binding domains is essential for its broad lytic activity. Virol. Sin. 30, 45–51, doi: 10.1007/s12250-014-3535-6 (2015).
Payne, K., Sun, Q., Sacchettini, J. & Hatfull, G. F. Mycobacteriophage Lysin B is a novel mycolylarabinogalactan esterase. Mol. Microbiol. 73, 367–381, doi: 10.1111/j.1365-2958.2009.06775.x (2009).
Rossi, P. et al. Structural elucidation of the Cys-His-Glu-Asn proteolytic relay in the secreted CHAP domain enzyme from the human pathogen Staphylococcus saprophyticus . Proteins 74, 515–519, doi: 10.1002/prot.22267 (2009).
Keen, E. F. 3rd et al. Prevalence of multidrug-resistant organisms recovered at a military burn center. Burns 36, 819–825, doi: 10.1016/j.burns.2009.10.013 (2010).
Church, D., Elsayed, S., Reid, O., Winston, B. & Lindsay, R. Burn wound infections. Clin. Microbiol. Rev. 19, 403–434, doi: 10.1128/CMR.19.2.403-434.2006 (2006).
Idelevich, E. A. et al. In vitro activity against Staphylococcus aureus of a novel antimicrobial agent, PRF-119, a recombinant chimeric bacteriophage endolysin. Antimicrob. Agents Chemother. 55, 4416–4419, doi: 10.1128/AAC.00217-11 (2011).
Mao, J., Schmelcher, M., Harty, W. J., Foster-Frey, J. & Donovan, D. M. Chimeric Ply187 endolysin kills Staphylococcus aureus more effectively than the parental enzyme. FEMS Microbiol. Lett. 342, 30–36, doi: 10.1111/1574-6968.12104 (2013).
Fernandes, S. et al. Novel chimerical endolysins with broad antimicrobial activity against methicillin-resistant Staphylococcus aureus . Microbial. Drug Resist. 18, 333–343, doi: 10.1089/mdr.2012.0025 (2012).
George, S. E. et al. Biochemical characterization and evaluation of cytotoxicity of antistaphylococcal chimeric protein P128. BMC Res. Note 5, 280, doi: 10.1186/1756-0500-5-280 (2012).
Loessner, M. J., Gaeng, S. & Scherer, S. Evidence for a holin-like protein gene fully embedded out of frame in the endolysin gene of Staphylococcus aureus bacteriophage 187. J. Bacteriol. 181, 4452–4460 (1999).
Eugster, M. R. & Loessner, M. J. Wall teichoic acids restrict access of bacteriophage endolysin Ply118, Ply511, and PlyP40 cell wall binding domains to the Listeria monocytogenes peptidoglycan. J. Bacteriol. 194, 6498–6506, doi: 10.1128/JB.00808-12JB.00808-12 (2012).
Cheng, Q., Nelson, D., Zhu, S. & Fischetti, V. A. Removal of group B streptococci colonizing the vagina and oropharynx of mice with a bacteriophage lytic enzyme. Antimicrob. Agents Chemother. 49, 111–117, doi: 10.1128/AAC.49.1.111-117.2005 (2005).
Nelson, D., Schuch, R., Chahales, P., Zhu, S. & Fischetti, V. A. PlyC: A multimeric bacteriophage lysin. Proc. Natl. Acad. Sci. USA 103, 10765–10770, doi: 10.1073/pnas.0604521103 (2006).
Lai, M. J. et al. Antibacterial activity of Acinetobacter baumannii phage varphiAB2 endolysin (LysAB2) against both gram-positive and gram-negative bacteria. Appl. Microbiol. Biotechnol. 90, 529–539, doi: 10.1007/s00253-011-3104-y (2011).
Chan, W. T., Verma, C. S., Lane, D. P. & Gan, S. K. A comparison and optimization of methods and factors affecting the transformation of Escherichia coli . Bioscience Rep. 33, doi: 10.1042/BSR20130098 (2013).
Yang, H. et al. Existence of separate domains in lysin PlyG for recognizing Bacillus anthracis spores and vegetative cells. Antimicrob. Agents Chemother. 56, 5031–5039, doi: 10.1128/AAC.00891-12AAC.00891-12 (2012).
Nelson, D., Loomis, L. & Fischetti, V. A. Prevention and elimination of upper respiratory colonization of mice by group A streptococci by using a bacteriophage lytic enzyme. Proc. Natl. Acad. Sci. U S A 98, 4107–4112, doi: 10.1073/pnas.061038398 (2001).
Yoong, P., Schuch, R., Nelson, D. & Fischetti, V. A. PlyPH, a bacteriolytic enzyme with a broad pH range of activity and lytic action against Bacillus anthracis . J. Bacteriol. 188, 2711–2714, doi: 10.1128/JB.188.7.2711-2714.2006 (2006).
Mataraci, E. & Dosler, S. In vitro activities of antibiotics and antimicrobial cationic peptides alone and in combination against methicillin resistance Staphylococcus aureus biofilms. Antimicrob. Agents Chemother. 56, 6366–6371, doi: 10.1128/AAC.01180-12 (2012).
Croes, S. et al. Staphylococcus aureus biofilm formation at the physiologic glucose concentration depends on the S. aureus lineage. BMC Microbiol. 9, 229, doi: 10.1186/1471-2180-9-229 (2009).
Brisbois, E. J. et al. Optimized polymeric film-based nitric oxide delivery inhibits bacterial growth in a mouse burn wound model. Acta Biomater. 10, 4136–4142, doi: 10.1016/j.actbio.2014.06.032S1742-7061(14)00288-8 (2014).
Lyskov, S. et al. Serverification of molecular modeling applications: the Rosetta Online Server that Includes Everyone (ROSIE). PloS one 8, e63906, doi: 10.1371/journal.pone.0063906 (2013).
Emsley, P. & Cowtan, K. Coot: model-building tools for molecular graphics. Acta Crystallogr. D 60, 2126–2132, doi: 10.1107/S0907444904019158 (2004).
Chen, V. B. et al. MolProbity: all-atom structure validation for macromolecular crystallography. Acta Crystallogr. D 66, 12–21, doi: 10.1107/S0907444909042073 (2010).
We are grateful to Ms. Juan Min, Ms. Bichao Xu, and Dr. Xuefang An from the Core Facility and Technical Support of Wuhan Institute of Virology for their excellent technical support in microscopy and animal studies.
ClyF has been transferred to Wuhan Phagelux biotechnical company, in which H.P.W. and H.Y. have financial interests.
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Yang, H., Zhang, H., Wang, J. et al. A novel chimeric lysin with robust antibacterial activity against planktonic and biofilm methicillin-resistant Staphylococcus aureus. Sci Rep 7, 40182 (2017). https://doi.org/10.1038/srep40182
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