Abstract
Human lysozyme is a key component of the innate immune system, and recombinant forms of the enzyme represent promising leads in the search for therapeutic agents able to treat drug-resistant infections. The wild type protein, however, fails to participate effectively in clearance of certain infections due to inherent functional limitations. For example, wild type lysozymes are subject to electrostatic sequestration and inactivation by anionic biopolymers in the infected airway. A charge engineered variant of human lysozyme has recently been shown to possess improved antibacterial activity in the presence of disease associated inhibitory molecules. Here, the 2.04 Å crystal structure of this variant is presented along with an analysis that provides molecular level insights into the origins of the protein's enhanced performance. The charge engineered variant's two mutated amino acids exhibit stabilizing interactions with adjacent native residues, and from a global perspective, the mutations cause no gross structural perturbations or loss of stability. Importantly, the two substitutions dramatically expand the negative electrostatic potential that, in the wild type enzyme, is restricted to a small region near the catalytic residues. The net result is a reduction in the overall strength of the engineered enzyme's electrostatic potential field, and it appears that the specific nature of this remodeled field underlies the variant's reduced susceptibility to inhibition by anionic biopolymers.
Introduction
Chronic pulmonary infections are a major cause of patient morbidity and mortality in diseases ranging from cystic fibrosis (CF) to chronic obstructive pulmonary disease (COPD) and pneumonias. In CF, polymicrobial airway infections are established early, and by adulthood most patient airways are persistently colonized by the opportunistic pathogen Pseudomonas aeruginosa, the primary cause of patient mortality [1]. Although a complete understanding of CF pathology remains elusive, it is thought that increased viscoelasticity of the airway surface liquid and reduced mucociliary clearance facilitate the establishment of chronic bacterial infections [2]. In addition to physiological factors that favor the persistent nature of CF infections, drug-resistance is a critical issue for both Gram-negative P. aeruginosa [3], [4] and Gram-positive pathogens such as Staphylococcus aureus [5] and various streptococci [6]. To more effectively manage bacterial infections associated with CF and other diseases such as COPD and pneumonias, there is a critical need for next generation antibiotics capable of treating drug-resistant pathogens. In one approach to new therapies, genetically engineered antimicrobial proteins are being developed based on knowledge of the mechanisms by which innate immune factors sometimes fail.
Human lysozyme (hLYS) kills bacteria by catalytic hydrolysis of cell wall peptidoglycan, but also exhibits catalysis-independent antimicrobial properties [7]. Its dual functions result in a protein that attacks both Gram-positive and Gram-negative bacterial pathogens, and hLYS has been shown to be the most effective cationic anti-pseudomonal agent in human airway fluids [8], [9]. In principle, this antimicrobial profile suggests that recombinant hLYS could serve as a potent, protein therapeutic if delivered to the airway using inhalation technologies such as those developed for the FDA-approved, DNA-degrading enzyme Pulmozyme [10]. However, the failure of endogenous hLYS to effectively clear bacteria during chronic infections indicates that the wild type sequence suffers from some specific dysfunction in the infected lung environment. Understanding and mitigating the inherent functional limitations of wild type hLYS could facilitate development of novel, antimicrobial, enzyme therapies.
The cationic nature of hLYS is thought to play an important role in guiding the protein to the negatively charged surface of bacteria. The dense positive charge of hLYS, however, also represents an Achilles' heel, as the wild type enzyme can be sequestered and inactivated by alginate [11], a biofilm matrix component associated with mucoid P. aeruginosa lung infections [12]. Furthermore, lower respiratory tract infections drive a hyperinflammatory immune response, and subsequently cause the local accumulation of additional, densely charged, anionic biopolymers including F-actin, DNA, and mucin [13], [14]. In the infected lung, these biopolymers may exceed 1% wt/vol. Concentrated polyanions radically alter the electrostatic environment of airway surface liquid, and are thought to inhibit various cationic antimicrobial peptides and proteins [15]. This type of electrostatic sequestration has been experimentally demonstrated with hen egg white lysozyme [16], and variants of T4 phage lysozyme having fewer cationic residues exhibit a reduced propensity to complex with F-actin while retaining ∼50% antibacterial activity in phosphate buffered saline (PBS) [17]. Building upon these studies, we sought to develop genetically engineered lysozyme variants designed specifically for high level activity in the presence of various disease-associated, anionic biopolymers, and against both Gram-negative and Gram-positive bacterial species.
Results and Discussion
Enhanced Catalytic Function
In an effort to reduce the immunogenic potential of our prospective therapeutic enzymes, we employed a human protein scaffold as a starting template. Combinatorial libraries of charge engineered hLYS variants were designed using bioinformatics and structural analysis, and approximately 150,000 mutated enzymes were screened for bacteriolytic activity in the presence of inhibitory alginate polyanion. Among other functionally enhanced enzymes, the Arg101→Asp and Arg115→His double mutant was found to lyse bacteria effectively at alginate, mucin and DNA concentrations that inactivated wild type hLYS. Moreover, in the absence of inhibitory biopolymers, the mutations did not substantially impair the enzyme's Vmax or Km, had no effect on its in vitro anti-pseudomonal activity, and did not reduce lytic function [11]. Indeed, time course killing assays in a standard lysozyme activity buffer (66 mM phosphate, pH 6.24) revealed that the double mutant's non-inhibited kinetics were faster than those of wild type hLYS [11]. More recently, we have extended the inhibition assays to include actin, which is known to be a key inhibitor of therapeutic proteins relevant to lung infections [14], [17]. In these studies, we chose to focus on the Gram-positive lytic activity of hLYS, and we therefore employed the model organism Micrococcus luteus. Our kinetic analysis is the first direct, experimental demonstration that charge engineering can enhance lysozyme activity in the presence of inhibitory F-actin (Fig. 1). Thus, combinatorial mutation of hLYS combined with high throughput functional screening generated an enzyme variant with decreased net charge, reduced susceptibility to anionic biopolymer inhibition, and no loss of intrinsic bacteriolytic activity.
Structural and Sequence Analysis
To gain molecular level insight into the double mutant's enhanced function, we determined the protein's X-ray crystal structure. Analysis of the Matthews coefficient [18] suggests that there are 2 molecules per asymmetric unit, with a VM value of 2.33 Å3 Da−1. We selected a mutation-free hLYS structure, 1LZS, as a search model for molecular replacement studies, and subsequently identified a clear solution containing two protomers. To avoid model bias associated with the high degree of sequence identity between the wild type protein and the double mutant (98.5%), iterative-build composite omit maps were calculated (Fig. 2). The high quality electron density permitted direct modeling of the initial molecular replacement solution. The mutant residues at positions 101 and 115 of the protein sequence search model were initially defined as alanine residues. Side chains for Asp101 and His115 were substituted only after observing clear electron densities at the respective positions. Iterative model building and refinement to 2.04 Å resolution yielded a unit cell containing 2050 atoms in two protein chains and 237 water molecules, which was in excellent agreement with experimental diffraction data (Table 1).
Table 1. Data Collection and Refinement Statistics.
Data Collection | |
Space Group | P212121 |
Unit Cell Parameters (Å, °) | 42.42 63.79 111.08, 90 90 90 |
Matthews coefficient (Å3/Da) | 2.33 |
Solvent content (%) | 46.9 |
Resolutiona | 19.86–2.04 (2.14–2.04) |
Total reflectionsa | 134735 (16297) |
Unique reflectionsa | 19829 (2606) |
Rsym (%)a b | 6.5 (18.6) |
Completenessa(%) | 99.7 (99.5) |
I/σIa | 21.6 (9.5) |
Refinement Statistics | |
# protein atoms (non-H) | 2050 |
# waters | 237 |
Rwork (%)a | 18.1 (17.7) |
Rfree (%)a | 22.2 (22.9) |
Ramachandran plotc (%) | 97.7/2.3/0 |
RMSD (Bonds/Angles) (Å, °) | 0.008/1.014 |
Average Isotropic B-factors (Å2) | |
Main chain (A/B)d | 14.91/15.08 |
Side Chain (A/B)d | 18.36/17.64 |
Waters | 22.43 |
Values in parentheses indicate statistics for the highest resolution shell of data;
Rsym = Σhj|Îh−Ihj|/ΣhjIhj;
Favored/allowed/outliers;
Residual B factors (does not include the contribution to atomic displacements from translation, libration and screw-rotation displacement).
The Arg101→Asp and Arg115→His mutations result in minimal perturbation of the global enzyme structure, as demonstrated by a superposition of the double mutant model onto the crystal structure of wild type hLYS (Fig. 3a). The mutated residues are situated at opposite ends of the substrate-binding groove, and as a result they have little impact on the catalytic core of the active site (Fig. 3b). Both mutated residues are stabilized by conformation specific interactions with native amino acids that are adjacent in space but distant in the primary sequence. The mutant Asp101 side chain forms an electrostatic N-O bridge [19] with Arg21, and is within hydrogen bonding distance of Tyr20 (Fig. 4a). Although the wild-type Arg101 side chain also forms a hydrogen bond with Tyr20, it does so with a geometry different from the mutant Asp101. Even more striking, repulsive charge-charge interactions cause the wild type Arg101 and neighboring Arg21 side chains to orient away from each other (Fig. 4b). At the second mutation site, the His115 side chain lies alongside Trp34 in a parallel displaced π-stacking interaction [20] (Fig. 2d). This orientation is similar to that of the wild type Arg115 side chain, and reproduces an interaction found among natural lysozymes having a histidine at this position, e.g. see canine milk lysozyme (PDB code 1QQY [21]).
A Consurf bioinformatics analysis [22] of 50, naturally occurring, C-type lysozyme orthologs was crucial in the development of the highly active double mutant [11], and a close examination of the results places the two performance-enhancing mutations within the context of natural lysozyme sequences. Using a multiple sequence alignment generated with the MUSCLE algorithm [23] (Fig. S1), the natural sequence variability of individual amino acid positions was assessed for the 50 lysozyme orthologs. A normalized evolutionary conservation score was then calculated for each of hLYS's 130 residues. The most highly conserved 25% of residues scored between −1.026 and −0.906, whereas the most poorly conserved 25% of residues scored between 0.589 and 2.811 (Fig. S2). In the multiple sequence alignment, residue 101 is occupied by an arginine in 24 cases, a serine in 24 cases, and a leucine or gap in the remaining two enzymes (Fig. S1). Despite the limited amino acid diversity at position 101, the lack of a clear consensus translates to a low degree of evolutionary conservation (normalized score = 0.895, least-conserved quartile). Significantly, the Asp101 side chain of our highly active double mutant forms multiple stabilizing interactions with neighboring amino acids (Fig. 4a), even though this residue does not naturally occur at position 101 among orthologs of our bioinformatics analysis (Fig. S1).
In contrast to position 101, position 115 was a consensus histidine in 38 of the lysozyme orthologs. In addition to the 38 enzymes possessing a consensus histidine, four orthologs encode Lys115, four Arg115, two Trp115, one Asn115, and one Gln115 (Fig. S1). The comparatively large stereochemical diversity among alternative residues at this site resulted in a low degree of evolutionary conservation (normalized score = 0.733, least-conserved quartile) similar to that of position 101. Notably, our highly active double mutant substitutes the wild type Arg115 with a consensus histidine. It is therefore not surprising that the mutant His115 side chain exhibits an energetically favorable interaction with at least one neighboring side chain (Fig. 2d).
Electrostatic Potential Analysis
The propensity for wild type hLYS to complex with and be inhibited by anionic biopolymers is due in large part to Coulombic interactions, and as expected the functionally enhanced double mutant has reduced cationic character. The calculated isoelectric point of wild type hLYS is 9.3, and its predicted net charge at neutral pH is +7.8 (Vector NTI sequence analysis software, Invitrogen, Carlsbad, CA). The corresponding values of the double mutant are 8.9 and +4.9, respectively. Thus, the two mutations should result in a substantial reduction in net charge near physiological pH, although the proteins were not clearly resolved on pH 3–10 isoelectric focusing gels (data not shown). To visualize the basis for the double mutant's enhanced performance in greater detail, we calculated the molecule's electrostatic potential field and compared the result to an identical analysis of the wild type structure. Consistent with the net charge shift, the overall strength of the double mutant's potential field is substantially decreased relative to wild type hLYS. At the same time, the two mutations manifest an expanded negative potential field in and around the substrate binding cleft (compare Fig. 3c and 3d). Despite these considerable changes, small portions of the double mutant's positive potential field have been maintained at wild type strength.
Stability Analysis
The structural stability of therapeutic proteins can play a key role in (i) preventing aggregation during storage and (ii) enhancing efficacy by preventing in vivo degradation. We therefore sought to assess the extent to which the Arg101→Asp and Arg115→His mutations influenced lysozyme stability. Thermal denaturation studies of the double mutant and wild type enzymes were conducted by differential scanning fluorimetry [24]. In PBS pH 7.4, wild type hLYS had a Tm = 63.7±0.6°C and the engineered double mutant had a Tm = 63.8±0.7°C. Thus, the two mutations had no significant effect on the engineered enzyme's thermal stability (p = 0.45).
In addition to thermal stability, resistance to human neutrophil proteases is an important parameter for pulmonary biotherapies, as neutrophil derived proteases can accumulate to micromolar concentrations in the infected and inflamed lung [25]. We therefore assessed proteolysis of the double mutant and wild type hLYS by human neutrophil elastase, cathepsin G, and proteinase 3. Our analysis shows that neither enzyme is susceptible to degradation by physiologically relevant concentrations of the three neutrophil proteases (Fig. 5). Combined with the thermal denaturation studies, these results indicate that the Arg101→Asp and Arg115→His mutations do not alter the double mutant's structural stability relative to wild type hLYS.
Conclusion
The double mutant detailed in this manuscript is not the only functionally enhanced enzyme to be isolated in the course of large combinatorial library screens. More than 30 different charge modified variants having diverse sequences, net charges, and charge distributions were found to exhibit greater lytic activity than wild type hLYS in the presence of inhibitory alginate biopolymer [11]. The Arg101→Asp and Arg115→His double mutant, however, is the only variant thus far proven to retain wild type or better lytic activity in the absence of inhibitory biopolymers (Fig. 1). This observation underscores the complex interplay between hLYS charge distribution and bacteriolytic function, and it suggests that specific regions of stereochemical conservation are key to engineering lysozymes with high level activity in both inhibitory and non-inhibitory conditions.
In summary, we have engineered the first lysozyme protein specifically designed for enhanced function in the presence of disease-associated, anionic biopolymers. This biotherapeutic candidate kills both Gram-negative (P. aeruginosa) and Gram-positive (M. luteus) bacteria more efficiently than the wild type protein under inhibitory conditions, and our structural analysis indicates that a reshaped electrostatic potential field underlies its enhanced antibacterial properties. The substituted amino acids of the variant enzyme exhibit energetically favorable interactions with spatially adjacent amino acids, and as a result the global structure and stability of the variant are equivalent to those of the wild type protein. While the charge engineered hLYS variant is particularly relevant to CF-associated bacterial infections, its broad spectrum utility may ultimately extend to other chronic or acute lung infections resulting from COPD, hospital acquired pneumonia or community acquired pneumonia.
Materials and Methods
Recombinant hLYS, freeze-dried M. luteus, and SYPRO Orange 5000× Protein Stain were purchased from Sigma-Aldrich (St. Louis, MO). MicroAmp® Fast Optical 0.1 ml 96-Well Plates and MicroAmp® Optical Adhesive Film were from Applied Biosystems (Bedford, MA). Human neutrophil elastase, human neutrophil cathepsin G, and human neutrophil proteinase 3 were from Athens Research & Technology (Athens, GA). Rabbit muscle G-actin was a kind gift from Dr. Henry N. Higgs and Ernest G. Heimsath, Jr. of Dartmouth College. All other chemicals and reagents were purchased from Fisher Scientific (Pittsburgh, PA).
Lysozyme Inhibition Assay
Time course lysis of Micrococcus luteus bacteria was monitored by light scattering at 450 nm, and specific rates of lysis with and without F-actin are reported. Light scattering was monitored in clear bottom 96-well plates on a Molecular Devices SpectraMax 190 UV/Vis microplate spectrophotometer. Non-inhibited reactions contained 300 µg/ml M. luteus and 200 ng/ml lysozyme in 150 µl of 5 mM Tris pH 7.0. Reactions with F-actin were assembled as follows: 120 µl solutions of rabbit muscle G-actin were polymerized by agitating at 25°C for 15 minutes in 50 mM KCl, 2 mM MgCl2, 0.2 mM CaCl2, 1 mM ATP, and 5 mM Tris pH 7.0. Thirty nanograms of purified lysozyme in 5 µl of 5 mM Tris pH 7.0 were then added to the F-actin solutions, and agitation was continued for an additional 20 minutes. Lytic reactions were initiated by adding 25 µl of 1.8 mg/ml M. luteus stock solution. The final actin concentration in the lytic reactions was 836 µg/ml. All lytic rates were determined from slopes of the initial, linear portions of light scattering vs. time data. Reactions were performed in triplicate, and repeated experiments yielded essentially identical results. The double mutant kinetics were also 2-fold faster than wild type hLYS in F-actin reactions containing 333 ng/ml lysozyme (data not shown).
Thermal Denaturation Studies
Differential Scanning Fluorimetry was performed essentially as described [24] using an ABI 7500 Fast Real-Time PCR System from Applied Biosystems (Bedford, MA). Proteins and SYPRO Orange were diluted in PBS. Final protein concentrations were 100 µg/ml and 50 µg/ml, and final dye concentrations were 20×, 10×, and 5×. Twenty µl reactions of all conditions (6 per protein) were performed in triplicate. The PCR gradient was run from 25–94°C with a 1 minute equilibration at each degree. Fluorescence was quantified using the preset TAMRA parameters. Melting temperatures were determined by data analysis with the “DSF Analysis v3.0.xlsx” Excel sheet (ftp://ftp.sgc.ox.ac.uk/pub/biophysics/) and GraphPad Prism v. 4 software (La Jolla, CA).
Proteolytic Sensitivity Assays
Wild type hLYS, the purified double mutant, or BSA were diluted to 90 ng/µl in 10 µl reactions containing either elastase, cathepsin G, or proteinase 3. Three final protease concentrations were examined: 0.5 ng/µl, 5 ng/µl, and 50 ng/µl. All assays were conducted in PBS pH 7.4. Reactions were incubated for 3 hours at 37°C, and the products were immediately analyzed on 15% reducing, denaturing, SDS-PAGE gels. Bands were visualized with Code Blue gel stain.
Crystallization and Data Collection
The isolation, expression, and purification of the mutated protein has been described in detail elsewhere [11]. Purified protein was dialyzed against crystallization buffer (10 mM KHPO4 pH 6.0, 100 mM NaCl) and concentrated to 7.0 mg/ml by centrifugal ultrafiltration. The protein was crystallized by 3–4 days of vapor diffusion against 20 mM sodium acetate pH 4.3, and 1.25 M NaCl at 18°C. The resulting crystals were cryoprotected by washing in mineral oil followed by soaking in well solution supplemented with 20% Ethylene Glycol. A complete dataset was collected for a single crystal at 100 K on a MAR345 image plate system using Cu Kα radiation produced with a rotating anode (Rigaku) equipped with focusing mirrors (Xenocs FOX-2D) and a Crystal Cryocooler (Cryo Industries).
Model Building and Refinement
Data reduction, indexing, integration and scaling were done using programs of the XDS package [26]. Since the protein crystal exhibited non-crystallographic symmetry (NCS), the Rfree set was selected in thin shells using the program SFTOOLS of the CCP4 package [27], and the same Rfree dataset was used throughout refinement. Owing to the availability of numerous homologous hLYS structures, we used molecular replacement to obtain the initial phases. Wild type hLYS (PDB code: 1LZS [28]) was employed as a search model in the AutoMR program of the PHENIX software suite [29]. A clear solution was found with a log-likelihood gain of 2508 and a solvent content of 46.9%, as determined from the Matthew's coefficient calculation. The AutoBuild module of the PHENIX suite was used to calculate a density-modified, NCS-averaged, solvent-flattened, histogram-matched, iterative build omit map, and the initial model was built into this omit map manually using the program COOT [30]. The solution was then subjected to multiple rounds of refinement using the Refine module of PHENIX. This process included rigid body refinement, individual and grouped B-factor refinement, and NCS averaging. When the model was well-refined, water molecules were picked and refined. Any water molecules exhibiting weak electron density or instability during refinement were subsequently discarded. TLS refinement using each chain as a TLS group was carried out in the final stages of refinement.
Protein Databank accession number
The atomic coordinates and structure factors of the double mutant have been deposited in the Protein Data Bank under accession number 3LN2.
Supporting Information
Acknowledgments
We would like to thank Dr. Brian Eckenroth for assistance collecting diffraction data at the University of Vermont, and Heather Jewell for general assistance optimizing methods for inhibition assays. Rabbit muscle actin was a kind gift of Dr. Henry N. Higgs and Ernest G. Heimsath, Jr., both of the Dartmouth Medical School Department of Biochemistry.
Footnotes
Competing Interests: KEG and TCS have filed a patent application on the therapeutic applications of the engineered human lysozyme. PCT/US10/21363 entitled “Therepeutic Charge Engineered Variants of Lysozyme and Methods for Using the Same to Treat Infections” was filed on January 16, 2010. This patent application does not alter the authors' willingness to adhere to all the PLoS ONE policies on sharing data and materials.
Funding: This work was supported by a Wallace H. Coulter Foundation (http://www.whcf.org/) Early Career Award, a Cystic Fibrosis Foundation (http://www.cff.org/) Carol Basbaum Memorial Postdoctoral Fellowship (SCANLO08F0), and P20RR018787-06 from the National Center for Research Resources (NCRR), a component of the National Institutes of Health. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
References
- 1.Govan JR, Nelson JW. Microbiology of lung infection in cystic fibrosis. Br Med Bull. 1992;48:912–930. doi: 10.1093/oxfordjournals.bmb.a072585. [DOI] [PubMed] [Google Scholar]
- 2.Rubin BK. Mucus structure and properties in cystic fibrosis. Paediatric Respiratory Reviews. 2007;8:4–7. doi: 10.1016/j.prrv.2007.02.004. [DOI] [PubMed] [Google Scholar]
- 3.Anderson GG, Moreau-Marquis S, Stanton BA, O'Toole GA. In Vitro Analysis of Tobramycin-Treated Pseudomonas aeruginosa Biofilms on Cystic Fibrosis-Derived Airway Epithelial Cells. Infect Immun. 2008;76:1423–1433. doi: 10.1128/IAI.01373-07. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 4.Projan SJ. (Genome) size matters. Antimicrobial Agents and Chemotherapy. 2007;51:1133–1134. doi: 10.1128/AAC.01370-06. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 5.Gibson RL, Burns JL, Ramsey BW. Pathophysiology and management of pulmonary infections in cystic fibrosis. Am J Respir Crit Care Med. 2003;168:918–951. doi: 10.1164/rccm.200304-505SO. [DOI] [PubMed] [Google Scholar]
- 6.Sibley CD, Parkins MD, Rabin HR, Duan K, Norgaard JC, et al. A polymicrobial perspective of pulmonary infections exposes an enigmatic pathogen in cystic fibrosis patients. Proceedings of the National Academy of Sciences. 2008;105:15070–15075. doi: 10.1073/pnas.0804326105. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 7.Nash JA, Ballard TNS, Weaver TE, Akinbi HT. The Peptidoglycan-Degrading Property of Lysozyme Is Not Required for Bactericidal Activity In Vivo. J Immunol. 2006;177:519–526. doi: 10.4049/jimmunol.177.1.519. [DOI] [PubMed] [Google Scholar]
- 8.Cole AM, Liao H-I, Stuchlik O, Tilan J, Pohl J, et al. Cationic Polypeptides Are Required for Antibacterial Activity of Human Airway Fluid. J Immunol. 2002;169:6985–6991. doi: 10.4049/jimmunol.169.12.6985. [DOI] [PubMed] [Google Scholar]
- 9.Travis SM, Conway BAD, Zabner J, Smith JJ, Anderson NN, et al. Activity of abundant antimicrobials of the human airway. American Journal of Respiratory Cell and Molecular Biology. 1999;20:872–879. doi: 10.1165/ajrcmb.20.5.3572. [DOI] [PubMed] [Google Scholar]
- 10.Shire SJ. Stability Characterization and Formulation Development of Recombinant Human Deoxyribonuclease I [Pulmozyme® (Dornase Alpha)]. In: Pearlman R, Wang YJ, editors. Pharmaceutical Biotechnology. New York: New York Kluwer Academic Publishers; 1996. pp. 393–426. [DOI] [PubMed] [Google Scholar]
- 11.Scanlon TC, Teneback CC, Gill A, Bement JL, Lamppa JW, et al. Enhanced antimicrobial activity of engineered human lysozyme. ACS Chemical Biology. 2010;5:809–818. doi: 10.1021/cb1001119. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 12.Ramsey DM, Wozniak DJ. Understanding the control of Pseudomonas aeruginosa alginate synthesis and the prospects for management of chronic infections in cystic fibrosis. Molecular Microbiology. 2005;56:309–322. doi: 10.1111/j.1365-2958.2005.04552.x. [DOI] [PubMed] [Google Scholar]
- 13.Rogers DF. Physiology of airway mucus secretion and pathophysiology of hypersecretion. Respiratory Care. 2007;52:1134–1149. [PubMed] [Google Scholar]
- 14.Ulmer JS, Herzka A, Toy KJ, Baker DL, Dodge AH, et al. Engineering actin-resistant human DNase I for treatment of cystic fibrosis. Proceedings of the National Academy of Sciences of the United States of America. 1996;93:8225–8229. doi: 10.1073/pnas.93.16.8225. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 15.Weiner DJ, Bucki R, Janmey PA. The Antimicrobial Activity of the Cathelicidin LL37 Is Inhibited by F-actin Bundles and Restored by Gelsolin. Am J Respir Cell Mol Biol. 2003;28:738–745. doi: 10.1165/rcmb.2002-0191OC. [DOI] [PubMed] [Google Scholar]
- 16.Sanders LK, Guáqueta C, Angelini TE, Lee J-W, Slimmer SC, et al. Structure and Stability of Self-Assembled Actin-Lysozyme Complexes in Salty Water. Physical Review Letters. 2005;95:108302. doi: 10.1103/PhysRevLett.95.108302. [DOI] [PubMed] [Google Scholar]
- 17.Sanders LK, Xian W, Guaqueta C, Strohman MJ, Vrasich CR, et al. Control of electrostatic interactions between F-actin and genetically modified lysozyme in aqueous media. Proceedings of the National Academy of Sciences. 2007;104:15994–15999. doi: 10.1073/pnas.0705898104. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 18.Matthews BW. Solvent content of protein crystals. J Mol Biol. 1968;33:491–497. doi: 10.1016/0022-2836(68)90205-2. [DOI] [PubMed] [Google Scholar]
- 19.Kumar S, Nussinov R. Close-Range Electrostatic Interactions in Proteins. ChemBioChem. 2002;3:604–617. doi: 10.1002/1439-7633(20020703)3:7<604::AID-CBIC604>3.0.CO;2-X. [DOI] [PubMed] [Google Scholar]
- 20.McGaughey GB, Gagne M, Rappe AK. Pi-Stacking Interactions: ALIVE AND WELL IN PROTEINS. Journal of Biological Chemistry. 1998;273:15458–15463. doi: 10.1074/jbc.273.25.15458. [DOI] [PubMed] [Google Scholar]
- 21.Koshiba T, Yao M, Kobashigawa Y, Demura M, Nakagawa A, et al. Structure and Thermodynamics of the Extraordinarily Stable Molten Globule State of Canine Milk Lysozyme†,‡. Biochemistry. 2000;39:3248–3257. doi: 10.1021/bi991525a. [DOI] [PubMed] [Google Scholar]
- 22.Landau M, Mayrose I, Rosenberg Y, Glaser F, Martz E, et al. ConSurf 2005: the projection of evolutionary conservation scores of residues on protein structures. Nucl Acids Res. 2005;33:W299–302. doi: 10.1093/nar/gki370. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 23.Edgar RC. MUSCLE: multiple sequence alignment with high accuracy and high throughput. Nucleic Acids Research. 2004;32:1792–1797. doi: 10.1093/nar/gkh340. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 24.Niesen FH, Berglund H, Vedadi M. The use of differential scanning fluorimetry to detect ligand interactions that promote protein stability. Nat Protocols. 2007;2:2212–2221. doi: 10.1038/nprot.2007.321. [DOI] [PubMed] [Google Scholar]
- 25.Voynow JA, Fischer BM, Zheng S. Proteases and cystic fibrosis. The International Journal of Biochemistry & Cell Biology. 2008;40:1238–1245. doi: 10.1016/j.biocel.2008.03.003. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 26.Kabsch W. Automatic processing of rotation diffraction data from crystals of initially unknown symmetry and cell constants. Journal of Applied Crystallography. 1993;26:795–800. [Google Scholar]
- 27.Collaborative Computational Project N. The CCP4 Suite: Programs for Protein Crystallography. Acta Crystallogr D Biol Crystallogr. 1994;D50:760–763. doi: 10.1107/S0907444994003112. [DOI] [PubMed] [Google Scholar]
- 28.Song H, Inaka K, Maenaka K, Matsushima M. Structural Changes of Active Site Cleft and Different Saccharide Binding Modes in Human Lysozyme Co-crystallized with Hexa-N-acetyl-chitohexaose at pH 4.0. Journal of Molecular Biology. 1994;244:522–540. doi: 10.1006/jmbi.1994.1750. [DOI] [PubMed] [Google Scholar]
- 29.Adams PD, Grosse-Kunstleve RW, Hung L-W, Ioerger TR, McCoy AJ, et al. PHENIX: building new software for automated crystallographic structure determination. Acta Crystallogr D. 2002;58:1948–1954. doi: 10.1107/s0907444902016657. [DOI] [PubMed] [Google Scholar]
- 30.Emsley P, Cowtan K. Coot: model-building tools for molecular graphics. Acta Crystallogr D. 2004;60:2126–2132. doi: 10.1107/S0907444904019158. [DOI] [PubMed] [Google Scholar]
- 31.Pettersen EF, Goddard TD, Huang CC, Couch GS, Greenblatt DM, et al. UCSF Chimera - A visualization system for exploratory research and analysis. Journal of Computational Chemistry. 2004;25:1605–1612. doi: 10.1002/jcc.20084. [DOI] [PubMed] [Google Scholar]
- 32.Higo J, Nakasako M. Hydration structure of human lysozyme investigated by molecular dynamics simulation and cryogenic X-ray crystal structure analyses: On the correlation between crystal water sites, solvent density, and solvent dipole. Journal of Computational Chemistry. 2002;23:1323–1336. doi: 10.1002/jcc.10100. [DOI] [PubMed] [Google Scholar]
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