To address the escalating problem of antimicrobial resistance and the dwindling antimicrobial pipeline, we have developed a library of novel aerosolizable silver-based antimicrobials, particularly for the treatment of pulmonary infections. To rapidly screen this library and identify promising candidates, we have devised a novel in vitro metric, named the “drug efficacy metric” (DEM), which integrates both the antibacterial activity and the on-target, host cell cytotoxicity. DEMs calculated using an on-target human bronchial epithelial cell-line correlates well (R2 > 0.99) with in vivo efficacy, as measured by median survival hours in a Pseudomonas aeruginosa pneumonia mouse model following aerosolized antimicrobial treatment. In contrast, DEMs derived using off-target primary human dermal fibroblasts correlate poorly (R2 = 0.0595), which confirms our hypothesis. SCC1 and SCC22 have been identified as promising drug candidates through these studies, and SCC22 demonstrates a dose-dependent survival advantage compared to sham treatment. Finally, silver-bearing biodegradable nanoparticles were predicted to exhibit excellent in vivo efficacy based on its in vitro DEM value, which was confirmed in our mouse pneumonia model. Thus, the DEM successfully predicted the efficacy of various silver-based antimicrobials, and may serve as an excellent tool for the rapid screening of potential antimicrobial candidates without the need for extensive animal experimentation.
Pseudomonas aeruginosa, a common gram-negative opportunistic pathogen, causes an estimated 51,000 serious healthcare-associated infections annually in the United States, and has been assigned a threat level of “serious” by the CDC1. Approximately 15% of these infections are caused by multidrug-resistant P. aeruginosa (MDR-PA), which are associated with worse overall clinical outcomes1,2. In particular, P. aeruginosa is one of the greatest causes of morbidity and mortality in pulmonary infections, such as ventilator-associated pneumonia (VAP) and chronic lung infections in patients suffering from cystic fibrosis (CF)3,4. The eradication of P. aeruginosa infection is particularly challenging due to its high degree of innate resistance to many antibiotic classes coupled with its ability to readily acquire additional resistance3,5,6. Similarly, other bacterial pathogens are also acquiring resistance rapidly, thereby turning antibiotic resistance in to a serious and growing global problem. Thus, to combat this problem, development of novel classes of antimicrobials is urgently required.
Silver (Ag) is particularly attractive as an antimicrobial candidate due to its excellent potency, broad spectrum activity, and low toxicity towards eukaryotic cells7,8,9,10. Few accounts of silver resistance have been reported and in most cases including P. aeruginosa, resistance to silver is transient and unstable, despite its widespread and continuous use11,12,13. Even though true, stable, silver resistance imparted through acquisition of plasmids or transposons has been documented in Salmonella Typhimurium and Escherichia coli14,15,16, few such strains exist, and no known reports of transmission of these components to P. aeruginosa exist17. However, poor bioavailability remains a significant challenge, because Ag+ cation, the bioactive form of silver, readily reacts with a wide range of physiological substrates and is rapidly rendered inactive11. Youngs et al. have synthesized N-heterocyclic silver carbene complexes (SCCs) with a diverse set of chemical structures and physico-chemical properties to overcome this challenge18,19,20,21,22,23,24. These SCCs provide gradual release of bioactive Ag+ from a stable silver complex, thus enabling retention of antimicrobial activity for prolonged periods in physiological conditions and sustaining its bioavailability19,20. For instance, the methylated caffeine-based SCC1 has served as one of the main candidates of interest, due to its moderate aqueous solubility and low toxicity21. SCCs derived using an imidazolium cation-based backbone, such as 4,5-dichloroimidazole, have also been synthesized due to their greater stability in aqueous solutions22; among these, some have been designed to be highly water soluble, such as SCC22 (up to 110 g/L)23, while others are highly lipophilic, such as SCC23 and SCC2825. Each of these SCCs has demonstrated broad spectrum antimicrobial activity against a diverse range of pathogenic bacteria in vitro18,19,20,21,23,24,25,26.
Our interest in the development of antimicrobials for the treatment of pulmonary bacterial infections has led us to explore aerosolization of SCCs, because this delivery method achieves higher local concentrations of drug in the lungs with reduced concern for systemic toxicity27. Our preliminary in vivo investigation has demonstrated the efficacy of SCC1 in a murine acute P. aeruginosa lung infection model21. Yet, an improvement in the pharmacokinetics of small molecule therapeutics such as the SCCs, delivered to the lung, can be achieved by employing formulations capable of providing sustained delivery at the target site27,28. Our previous work with SCC-loaded, L-tyrosine polyphosphate (LTP) and shell cross-linked knedel-like (SCK) nanoparticle formulations (NPs) for the treatment of P. aeruginosa lung infections has shown a survival advantage compared with sham treatment in our acute P. aeruginosa infection model with SCC doses far lower than those required of free drug to achieve the same clinical effect29,30.
While we have demonstrated efficacy of several silver-bearing antimicrobial formulations in vivo, we have explored only a small subset of the total possible formulations. The recent development of biodegradable polyphosphoester-based SCK NPs31 has further increased the number of available platforms for SCC delivery to the lung32. Therefore, a rational approach to identify promising candidates for in vivo efficacy and safety testing is needed. “Therapeutic index” (TI), a combined quantitative metric based on the relative in vivo safety and efficacy of a compound, appears to provide a convenient method for the identification of promising therapeutic candidates33. In this study, we have developed an in vitro adaptation of the therapeutic index, named the drug efficacy metric (DEM), which is effectively the ratio of the drug toxicity breakpoint (in vitro half-median lethal dose, i.e., LD50) and the drug potency breakpoint (in vitro minimum bactericidal concentration, i.e., MBC), i.e., LD50/MBC. Because our goal was to identify in vitro parameters that are predictive of in vivo antimicrobial efficacy, we have correlated in vitro metrics such as the DEM, minimum inhibitory concentration (MIC), MBC, and LD50 with median survival hours (a metric for in vivo efficacy) of P. aeruginosa infected mice following aerosolized treatment with SCCs. We hypothesized that the DEM would correlate the best with in vivo efficacy compared with other metrics such as the MIC, MBC, and LD50 alone and that SCCs with higher in vitro DEM values would demonstrate superior in vivo efficacy. Next, to validate our hypothesis that an on-target cell type is critical for the DEM to accurately predict in vivo efficacy, we have calculated the DEM using a human bronchial epithelial cells 16HBE (on-target) and primary human dermal fibroblasts HDFs (off-target) and correlated both DEMs to median survival hours. Next, in vivo dose-response studies were performed using the two most promising SCCs (SCC1 and SCC22) with the highest DEM to investigate whether increased doses of the SCCs lead to a better survival outcome. Lastly, we validate the predictive ability of the DEM, by demonstrating that the DEM is capable of predicting the in vivo efficacy of a silver-bearing nanoparticle formulation defined as median survival hours.
In vitro testing of silver-based antimicrobial formulations and determination of in vitro Drug Efficacy Metric (DEM)
The chemical structures of the four SCCs investigated in this manuscript and a summary of their antimicrobial activity is presented in Fig. 1. Initially, preliminary cytotoxicity screening of a subset of eight SCCs from a library of ~30 SCCs was performed using alamarBlue® against immortalized human bronchial epithelial cells (16HBE) to determine in vitro LD50 (Supplementary Figure S1). The four SCCs discussed here were chosen based on their divergence of chemical structures and in vitro cytotoxicity profile against 16HBEs. These four SCCs were evaluated for their antimicrobial activity against a representative mucoid clinical P. aeruginosa strain, PA M57-15, by determining their MIC and MBC. The hydrophobic, naphthalene containing 4,5-dichloroimidazole based SCC23 and SCC28 have comparable MICs against PA M57-15 on a molar basis (0.86 and 0.95 µM, respectively), while hydrophilic SCC22 and SCC1 have a slightly higher MIC at 2 µM (Fig. 1). With respect to the MBCs, even though SCC1 had the highest MBC (4 µM) and SCC23 had the lowest MBC (1.7 µM) on a molar basis, the MBCs for all four SCCs are almost identical and within experimental error on a µg/mL basis. Evaluation of Ag-PPE-SCKs against 16HBEs demonstrated an LD50 of 100 µM; whereas, the MBC against PA M57-15 was 0.188 µg/mL, based on silver mass, which is equivalent to that of SCC23 on a molar basis (~1.7 µM).
Based on the alamarBlue® cytotoxicity assay using 16HBEs, many of the SCCs have similar toxicity profiles; however, SCC23 and SCC28 based on a 4,5-dichloroimidazole backbone have notably higher toxicity with LD50 values of 14.7 and 58.1 µM respectively (Supplementary Figure S1 and Fig. 2A). On the other hand, SCC1, a methylated-caffeine based hydrophilic SCC has an LD50 of 297 µM and SCC22, a hydrophilic complex based on a 4,5-dichloroimidazole backbone has an LD50 of 224 µM, thus, suggesting the low toxicity of these compounds (Fig. 2A). When tested for toxicity against human dermal fibroblasts (HDFs), minimal differences were observed among the four SCCs with the LD50 values being 25.8, 22.7, 14.2, and 9.8 µM for SCC1, SCC22, SCC23, and SCC28, respectively (Fig. 2C). Furthermore, the LD50 values for SCC23 are comparable for 16HBEs and HDFs, while significant differences exist between the LD50 values for the two cell types with regards to the other SCCs. Finally, the Ag-PPE-SCKs were only tested against 16HBEs, yielding an average LD50 of 100 µM.
The DEM, which is the ratio of the in vitro LD50 to the in vitro MBC, was subsequently calculated for each SCC and Ag-PPE-SCKs. When comparing the SCCs via the DEM using 16HBEs, an on-target cell type, significant differentiation between the compounds was seen; SCC1 and SCC22 have significantly higher DEMs than SCC23 and SCC28 (Fig. 2B) as determined by ordinary one-way ANOVA with Tukey’s multiple comparisons test. However, SCC22 is not significantly higher in DEM than SCC1. Thus, the ranking of the SCCs determined by16HBE-based DEM values is SCC22 > SCC1≫ SCC28 > SCC23. Furthermore, the DEM of Ag-PPE-SCKs determined using 16HBEs is slightly lower than SCC1, but the difference is non-significant (P = 0.0528) as determined by unpaired t-test (Fig. 6). In contrast, when using HDFs, an off-target cell type, no distinct trends could be distinguished. SCC23 and SCC22 show slight and non-significant trends for the highest DEM (Fig. 2D), yet no significant differences can be found between DEM values for any of the SCCs (P > 0.05).
Aerosolized SCC22 and SCC1, but not SCC23 and SCC28, are efficacious in vivo in a mouse model of acute P. aeruginosa pneumonia
The antimicrobial efficacy of SCC1, SCC22, SCC23, and SCC28 have been tested side-by-side as nebulized treatments in a mouse model of acute P. aeruginosa lung infection. Of the 25 μmol of the SCCs delivered into the multi-dosing chamber, approximately 1% is delivered to the lungs of each mouse as demonstrated by our previous biodistribution data34,35, which results in an effective silver (Ag+) dose of ~1.3 mg/kg or 27.3 μg per mouse per dose. The mice treated with SCC22 resulted in a superior survival of 42% compared to sham (9.1%, P ≤ 0.05), while those treated with SCC1 demonstrated a 25% survival, thus demonstrating a survival trend compared with sham treatment (P = 0.0831) (Fig. 3A). In contrast, mice treated with SCC23 and SCC28 had significantly lower survival compared with mice administered sham treatment (P ≤ 0.05), as well as mice administered SCC22 and SCC1 treatments (P ≤ 0.001; Fig. 3A). None of the treatments had a significant effect on mouse weight throughout the 96 hours of the study (Fig. 3C), though the SCC1 and SCC22 treated mice showed significantly lower signs of illness at 24 hours following infection (P = 0.0378 and 0.0060, respectively) (Fig. 3D). Furthermore, the mice treated with SCC23 appeared the most infirm at each time-point based on the clinical illness scores. However, the investigators assigning the scores were not blinded to the treatment group, which is a limitation of this study.
Histological examination of lung tissue following aerosolized treatment with SCCs does not adequately correlate with in vivo outcome
Histological examination of the lungs of infected animals treated with nebulized SCCs or vehicle (sham) allowed differentiation into three tiers of increasingly abnormal appearance, but was unable to provide additional insights into the in vivo survival outcome. The lungs of mice treated with SCC22 (Fig. 4B) appeared less inflamed and abnormal than those of SCC1 (Fig. 4A), SCC23 (Fig. 4C) and SCC28 (Fig. 4D), which were less abnormal than the lungs of sham-treated mice (Fig. 4E,F). As expected, the lungs of vehicle-treated animals show dense, diffuse, and severe inflammatory infiltrate in both interstitial and intra-alveolar spaces with extensive areas of acute consolidation consistent with pneumonia. Furthermore, severe congestion and haemorrhage was also observed and consolidated areas also reveal abundant bacterial colonies. These mice exhibited an aggregate histological score of +6 based on inflammation, consolidation, and haemorrhaging as parameters. In contrast, lungs of animals treated with SCC22 revealed mild, patchy interstitial mononuclear and polymorphonuclear inflammation with small, focal areas of parenchymal neutrophilic consolidation consistent with pneumonia. Even though vessels show mild congestion, no focal haemorrhage was observed and mice in this group had an aggregate histological score of +3. No bacterial colonies were identified in the tissue samples. Similarly, in the case of animals treated with SCC1, lung parenchyma shows mild-to-moderate inflammatory infiltrates with both mono- and polymorphonuclear cells and mild, patchy consolidation with complete absence of bacterial colonies. However, focal haemorrhages were identified along with mild vessel congestion and the mice in this group had an aggregate histological score of +4. In the case of SCC23 treated animals, mild-to-moderate polymorphonuclear neutrophilic inflammation in both interstitial areas and intra-alveolar spaces along with patchy, moderate consolidation, as well as mild congestion and haemorrhages were observed. These observations resulted in an aggregate histological score of +4 in the SCC23 treated mice. Of all SCC treatments, lungs of animals treated with SCC28 showed the highest degree of inflammation; a denser, moderate inflammatory interstitial and intra-alveolar infiltrate with predominantly polymorphonuclear neutrophils was observed. Additionally, patchy, moderate areas of consolidation and moderate parenchymal haemorrhages were also present. However, based on our semi-quantitative histopathological scoring system, the mice in this group had an aggregate score of 4, which is not different from the SCC1 and SCC23 groups. Nevertheless, bacterial colonies were not identified in the lung tissues of animals treated with either SCC23 or SCC28. Thus, histological scores allowed ranking of SCC efficacy as SCC22 > SCC1, SCC23, SCC28≫ sham.
Drug Efficacy Metric (DEM) derived using an on-target cell type provides the best measure of in vivo activity for silver-based antimicrobials
A Cox proportional hazards regression model was used to identify the in vitro parameter that demonstrates the best correlation with the probability of survival. All in vitro parameters, except HDF DEM (P = 0.0835), have a significant effect on survival (P < 0.0001). The R2 values listed in Table 1 demonstrate 16HBE DEM (R2 = 0.5166) to be the most effective predictor of survival probability of all the in vitro parameters tested in this study.
We have also utilized linear regression to correlate the median survival hours for the mice by SCC treatment with in vitro parameters for antimicrobial activity and toxicity, namely, MIC and MBC against PA M57-15, LD50 against eukaryotic cells (16HBEs and HDFs), and the DEM (LD50/MBC). Cell cytotoxicity, as measured by LD50 against the 16HBE cells, was fairly predictive of in vivo efficacy (R2 = 0.8773) (Fig. 5B) and SCCs with lower toxicity generally resulted in higher efficacy. On the other hand, cytotoxicity against HDFs was not as well correlated with survival (R2 = 0.7987) (Fig. 5E). When using antimicrobial potency, good correlation between in vitro MIC and in vivo efficacy was observed (R2 = 0.9753); however, the correlation with in vitro MBC was poor (R2 = 0.6283) (Fig. 5A,D). Furthermore, these correlations appear to be in a reverse order with less potent SCCs generally resulting in better survival. For instance, SCC23 has the lowest MBC (1.7 μM) of all 4 SCCs against PA M57-15, yet it yielded the worst survival outcome. On the other hand, SCC1 has the highest MBC (4.0 μM) among the 4 SCCs tested, yet it resulted in a survival advantage over sham treatment. When using the DEM, a combined metric based on in vitro antimicrobial activity (MBC) against PA M57-15 and in vitro cytotoxicity against 16HBEs, the best correlation with in vivo efficacy was observed (R2 = 0.9932, Fig. 5C). The correlative equation resulting from linear regression of this data is Y = 0.3777X + 31.97, where Y = median survival hours and X = mean DEM. Furthermore, as expected, the SCCs with higher DEMs resulted in superior in vivo efficacy. Interestingly, when 16HBEs were substituted with HDFs for cytotoxicity determination, however, the DEM correlation was very poor (R2 = 0.0595, Fig. 5F) underscoring the importance of the on-target cell type for DEM determination.
DEM predicts the in vivo efficacy of aerosolized Ag-PPE-SCKs
SCC1 and Ag-PPE-SCKs were compared head-to-head in our acute P. aeruginosa lung infection model due to their similar and statistically indifferent in vitro DEMs. Based on the DEM value for Ag-PPE-SCKs (mean DEM = 58.82), we predicted the median survival of mice in that group to be 54.2 hours, which translates to a survival of 50% of the cohort at 54.2 hours theoretically. In our experiments, we observed that both formulations yielded improved survival over sham treatment (P < 0.01) as determined by log-rank Mantel-Cox test (Fig. 6). The Ag-PPE-SCKs and SCC1 resulted in survival advantage of 58% and 50%, respectively compared with sham treatment. While the DEM generally would predict a slightly higher efficacy of SCC1 over the Ag-PPE-SCKs, the nanoparticles yielded slightly higher survival in vivo despite only being dosed twice 24 hours apart (Fig. 6). Even though we were unable to calculate the median survival hours for the Ag-PPE-SCK-treated mice for direct correlation with the DEM due to greater than 50% survival, the observation that at least 50% of mice in this cohort were alive at 54.2 hours validates the predictive ability of the DEM.
A dose response is observed for survival with SCC22, but not SCC1, in P. aeruginosa infected mice
SCC1 and SCC22, due to their highest in vitro DEM, that is least toxicity with highest efficacy, and their ability to confer survival advantage in the murine P. aeruginosa pneumonia model compared with sham treatment, were chosen for dose-response studies. Both compounds were tested in vivo at increasing dosages (25, 50, and 100 µmol), first in the presence of DMSO to further evaluate their antimicrobial efficacy and safety. Surprisingly, with DMSO in the solution, higher doses of SCCs exhibited lower survivals than lower doses of these compounds. For instance, with SCC1, the lowest dose (25 µmol) resulted in a 42% survival advantage; whereas, the highest dose (100 µmol) resulted in the lowest survival advantage of 17% compared with sham treatment (Supplementary Figure S2A). However, each dose provided a significant survival advantage over sham treatment (P ≤ 0.001). Similarly, SCC22 treatment at 25 and 50 µmol led to 58 and 50% survival advantage, respectively (P ≤ 0.05); however, the highest dose (100 µmol) did not yield any survival advantage over sham treatment (Supplementary Figure S2B). Next, these studies were repeated without DMSO in the solution to delineate the effects DMSO may have in this acute infection model when used in combination with SCCs. Interestingly, when the in vivo efficacy studies were performed using DMSO-free formulations of SCC1 (Fig. 7A), no definitive dose-response trend could be distinguished and the highest dose led to a slight, but non-significant improvement in survival advantage (100 µmol, 73%) compared to the two lower doses (50 µmol, 64%; 25 µmol, 58%). However, all three doses provided a significant survival advantage in comparison with sham treatment (P ≤ 0.01). On the other hand, when similar studies were performed using DMSO-free formulations of SCC22 (Fig. 7B), a well-defined correlation between therapeutic dose and efficacy was observed with the lowest dose (25 µmol) resulting in a 25% survival advantage and the two highest doses (50 and 100 µmol) providing a 67% survival advantage over sham treatment (P ≤ 0.001).
We, in collaboration with the Youngs and Wooley research groups, have developed a library of silver-based antimicrobial formulations including silver carbene complexes (SCCs) and silver-bearing biodegradable nanoparticles in response to the rapidly shrinking antimicrobial pipeline. In this work, we describe the in vitro drug efficacy metric (DEM) and demonstrate its superior correlation with in vivo survival for a subset of SCCs compared with other in vitro efficacy and toxicity parameters, thereby highlighting its utility in identifying efficacious yet safe silver-based antimicrobials for further studies. Further, we demonstrate that treatment with aerosolized Ag-PPE-SCKs, which have an in vitro DEM and therefore predicted in vivo efficacy comparable to SCC1, indeed provides a survival advantage comparable to SCC1 treatment. To our knowledge, the DEM described here is not only the first example of an in vitro metric that correlates very strongly with in vivo outcomes for a class of antimicrobials, but also the first example of a predictive correlation that has been developed for aerosolized antimicrobials. Furthermore, the assays used for the DEM are amenable to high throughput screening and would allow the rapid screening of a large library of compounds.
A few previous reports document in vitro metrics used to predict therapeutic indices for screening potential antimicrobial agents, particularly antimicrobial peptides36,37,38. Since these antimicrobials primarily function by damaging cell membranes39, the ratio of the minimal haemolytic concentration (MHC) against erythrocytes and the bacterial MIC (MHC/MIC) is a common metric used to predict in vivo efficacy40. However, this in vitro therapeutic index metric has yet to be demonstrated to reliably predict outcomes in vivo. In fact, Copple et al. state that the in vitro TI cannot be used to reliably predict in vivo outcomes41. Similar difficulties correlating in vitro cellular and bacterial toxicities of topical antimicrobials with in vivo efficacies have also been reported42,43,44,45. Recently, Müller and Kramer defined the term “biocompatibility index” (BI) for antiseptic agents, based on in vitro cytotoxicity against L929 murine fibroblasts and the antibacterial activity against Staphylococcus aureus and Escherichia coli46. BI greater than 1 is representative of an antiseptic substance with a more suitable efficacy-cytotoxicity profile than an antiseptic substance with BI less than 1. Even though the authors claim that the BI may more realistically mimic antiseptic action in vivo compared with previous indices, the absence of supporting in vivo correlative evidence is a shortcoming of this study. Other models relying on in vitro data to predict in vivo antimicrobial efficacy evaluate bacterial susceptibilities following drug exposure at concentrations predicted based on pharmacokinetics of the agent47,48,49. While useful in certain situations50, these models require pharmacokinetic data, which may be unavailable during early phases of drug development.
Our primary goal is to develop the silver-based antimicrobials as aerosolizable therapeutics. Considering the importance of developing indication specific tests with on-target cell types for the evaluation of cytotoxicity of drug candidates33,46, we initially performed cytotoxicity testing of SCCs using 16HBEs. We considered the use of primary tracheal epithelial cells grown at air-liquid interface; however, we have previously shown that the LD50 of primary cells exposed to SCC1 is about 2 log10 higher than that of 16HBE such that the amount of drug required for screening would have rendered the study impractical51. Secondary cytotoxicity studies with human fibroblasts were performed, not only because fibroblasts are commonly used for cytotoxicity studies, but also because we desired to explore the effect that an off-target cell type on the predictive capabilities of the DEM. The low toxicity of SCC1 with its methylated caffeine backbone is not surprising considering such xanthine derivatives have low toxicity and have been used for multiple purposes including bronchodilation52. Of the other three SCCs, which are all based on a 4,5-dichloroimidazole backbone, SCC23 and SCC28 are the most toxic, potentially due to the incorporation of naphthalene functionalities, a structural modification that was performed to increase hydrophobicity. The higher toxicities with these SCCs point towards the effect of their backbone substituents and suggest that by choosing safe carrier molecules, enhanced activity can be obtained while ensuring low toxicity.
The four SCCs investigated in this work demonstrated comparable potency based on their MICs and MBCs, as previously described. These results suggest that the antimicrobial activity is primarily due to the bioactive Ag+ cation and the carrier molecules appear to contribute minimally to antimicrobial activity. Next, we calculated the DEMs for each cell type using both 16HBEs and HDFs. As with the LD50 measurements, an excellent separation between the SCCs was observed when using 16HBEs, but a minimal separation was noted when using HDFs. Thus, based on the DEM data for 16HBEs, SCC1 and SCC22 appear to possess the best balance of efficacy versus cytotoxicity among the four SCCs; whereas, no such distinction can be made based on the DEM data for HDFs. Unfortunately, because of the comparable potency of all four SCCs against PA M57-15, the LD50 values appear to overly drive the DEM calculations, which is a drawback of this study.
The survival advantage observed in our murine P. aeruginosa pneumonia model following aerosolized SCC1 and SCC22 treatments, but not SCC23 and SCC28 treatments (Fig. 3), despite the excellent in vitro potency of SCC23 and SCC28, suggests a strong effect of drug toxicity during infection. To further elucidate this observation and determine whether the toxicity was localized to the lung tissue, we examined the lung tissue of PA M57-15 infected mice following SCC treatments. Histological examination of the lung tissue following concomitant SCC exposure in P. aeruginosa infected mice demonstrated a complete absence of bacterial colonies in all but sham-treated mice suggesting that all four SCCs exerted antimicrobial activity in vivo (Fig. 4). The superiority of SCC22 observed during survival studies was also reflected during histology studies. The lungs of SCC22 treated mice exhibited the lowest aggregate histopathological score suggesting a lower overall host-response possibly due to a combination of antimicrobial efficacy and low toxicity. Surprisingly, despite the low toxicity of SCC1 in vitro and the successful outcome observed with SCC1 treatment in our infection model, the lung tissue of these mice had a histopathological score comparable to the lung tissue of SCC23 and SCC28 treated mice. Furthermore, a lower degree of severity of host-response parameters was observed for SCC23 and SCC28 treatment compared with sham treatment, even though the survival outcome for these two treatments was worse. Overall, these results suggest a poor correlation between in vivo efficacy and histological data. A plausible explanation for the observations with SCC23 and SCC28 treatment could be due to the occurrence of additional downstream toxic effects induced by these compounds. While biodistribution studies performed using radiolabelled Ag+ show minimal accumulation of SCC1 and Ag-PPE-SCKs in the liver34, there is a likelihood that use of a different backbone, such as naphthalene-bearing, may alter the biodistribution of the SCCs and lead to its accumulation in the hepatic tissue causing toxicity, in addition to that directly observed in the lungs.
A Cox proportional hazards model demonstrates 16HBE DEM (R2 = 0.5166) to be the best predictor of survival followed by MIC (R2 = 0.5014). However, a major limitation of this model is that the hazard ratio (probability of death) is not dependent on time53. For instance, an increase in one order of magnitude 16HBE DEM and MIC reduces the log hazard rate by 0.0335 and 2.0282, respectively. Thus, this model merely demonstrates 16HBE DEM to be a better predictor of survival compared with other in vitro parameters, but fails to provide any insights into the effect of in vitro parameters on the survival time. This limitation was addressed by correlating the DEM to survival times using linear regression.
The correlation between in vitro efficacy and toxicity parameters including the combined DEM metric with in vivo efficacy exhibited a varied response (Fig. 5). While MIC, and not MBC, alone demonstrates a robust correlation with in vivo efficacy, both these parameters demonstrate a correlation in reverse order with survival. Therefore, even though lower MIC and MBC values indicate superior in vitro potency, they necessarily do not translate to in vivo efficacy. For instance, the MIC correlates the best statistically with survival hours (R2 = 0.9753); however, this correlation fails to actually show an in vivo response as expected. Based on the MIC vs. efficacy correlation, SCC23 and SCC28 should perform the best and result in the highest survival of mice; however, SCC23- and SCC28-treated mice exhibit a survival outcome that is worse than sham-treated animals. The LD50 for on-target 16HBEs demonstrated a better correlation with in vivo efficacy compared with the LD50 for off-target HDFs, yet the LD50 values for both cells demonstrated a direct correlation with survival, suggesting lower in vitro toxicity is indicative of a superior in vivo outcome. The combined DEM metric based on 16HBEs (R2 = 0.9932) demonstrates the second-best correlation with median survival hours along with a minor statistical difference compared with MIC. However, with regards to actual biological antimicrobial efficacy, this metric, which considers both the safety and efficacy of the drug candidates against an on-target cell type, exhibits the best correlation since the antimicrobial candidates with the highest DEM also exhibit the highest median survival hours. Similarly, preliminary studies also demonstrate a robust correlation between in vivo efficacy and the DEM when replacing PA M57-15 with another strain of P. aeruginosa (PA O1) for antimicrobial studies (data not shown). In contrast, the correlation with survival hours considerably worsened when using the same metric based on HDFs (R2 = 0.0595). These findings are noteworthy, not only because they validate our hypothesis, but also because of the distinction they provide between our DEM metric and the BI proposed by Müller and Kramer46. Even though both metrics are defined using essentially the same parameters (DEM = LD50/MBC vs. BI = IC50/MBC), the BI metric would have falsely predicted SCC23 and SCC28 to be safe since each SCC would have a BI > 1 (based on both 16HBE and HDF cytotoxicity data). In fact, based on BIs determined using off-target cells such as HDFs, SCC23 would have been incorrectly identified as a lead candidate, which in turn would have led to an extremely poor prediction of in vivo efficacy. Thus, an appropriate metric coupled with a judiciously chosen on-target cell type is critical for identifying efficacious, yet safe compounds.
One of our main goals was to identify in vitro parameters capable of predicting in vivo efficacy. Considering the excellent correlation between the in vitro 16HBE-based DEM and in vivo efficacy for the SCCs, we sought to explore whether the DEM would predict efficacy of another silver-based antimicrobial formulation, namely Ag-PPE-SCK NPs. Since both SCC1 and Ag-PPE-SCKs demonstrated comparable in vitro DEM values, they were compared head-to-head in our acute P. aeruginosa infection model and we observed a slightly better than predicted outcome with the Ag-PPE-SCKs (Fig. 6). The most likely reason for this outcome is the different pharmacokinetic profiles of SCCs, which distribute through the body quickly, and the nanoparticles, which reside in the lungs for longer periods of time and therefore provide a sustained delivery of the encapsulated SCC at the target site35. Because the DEM relies on a balance of cytotoxicity and efficacy in predicting in vivo efficacy without taking pharmacokinetics into account, the predictive capability is not as robust as with the SCCs. Thus, the data also point towards the importance of detailed pharmacokinetic (PK) studies as the essential next step in the development of new drug candidates and their formulations.
Our initial in vivo studies utilized DMSO for all SCC formulations owing to the lipophilic nature of SCC23 and SCC28 and the need to maintain consistency across all formulations, yet SCC1 and SCC22 are hydrophilic and do not require DMSO for solubilisation. Further, the presence of DMSO in our current studies led to a lower survival for infected SCC1-treated mice at similar doses (25 μmol) in the same acute lung infection model, compared to our previously published observation21. Additionally, the distinct survival advantage conferred using SCC1 and SCC22 even at a low dose (25 μmol) in the initial in vivo experiments sparked the motivation for the dose-response studies. Our goal for this set of experiments was to explore (a) the effects of DMSO on the efficacy of SCCs in our acute infection model and (b) the dose-response of SCC1 and SCC22. When comparing the efficacy of DMSO-containing (Figure S2) and DMSO-free (Fig. 7) SCC formulations at three doses (25, 50, and 100 μmol), each delivered by nebulization to P. aeruginosa infected mice, the use of DMSO appears to have more of an adverse effect on survival with SCC1 than SCC22. Further, in the presence of DMSO, higher doses of SCCs provide less therapeutic benefit than lower doses, and the differences in survival at higher doses are more pronounced for SCC22 than SCC1. These data indicate that DMSO artificially lowers the efficacy of both SCC1 and SCC22. DMSO, which is a known promoter of drug absorption54,55, may have led to an accelerated transport of SCCs from the lung epithelium into the systemic circulation causing a reduction in its local therapeutic potential. Furthermore, Pesanti and Nugent have demonstrated a dose-dependent inhibition of P. aeruginosa clearance in intratracheally infected mice following intraperitoneal administration of DMSO56. In addition, their data revealed that even a 10% solution of DMSO delivered intranasally, resulted in a detectable increase in susceptibility of mice to P. aeruginosa infection56. Even though the precise mechanisms related to this phenomenon are unknown, its occurrence may partially explain the observed reduction in efficacy of SCC1 and SCC22 when using DMSO. Furthermore, we speculate that both the transport- and clearance-related effects of DMSO may have contributed to the failure of SCC23 and SCC28 treatments in vivo in addition to their confirmed toxicity. Separately, both SCC1 and SCC22 provide a significant survival advantage over sham treatment and a distinct dose-response is observed for SCC22 but not SCC1, in the absence of DMSO. Interestingly, the only significant difference in survival is between the lowest dose of SCC22 and the two higher doses of SCC22 and the three doses of SCC1. Possibly, at higher doses, sufficient SCC22 is present in the lung to maintain therapeutic concentrations considerably higher than the MBC at all times. However, at the lowest dose, the SCC22 concentration may peak following treatment and gradually return to MBC or sub-MBC levels at later time-points, leading us to believe that the transport rate across the lung epithelium, as well as lung-retention of these compounds, may be different. This topic will form the basis of a separate investigation.
In summary, we have shown a robust correlation between the DEM derived using an on-target cell type and in vivo efficacy for aerosolized silver-based antimicrobials against P. aeruginosa as a model pathogen. While other parameters of in vitro efficacy and toxicity demonstrated a moderate-to-good correlation with in vivo efficacy, the correlation with the 16HBE-based DEM was the best, which validates our hypothesis. Surprisingly, histological data from the same P. aeruginosa infection model used for the survival studies, failed to correlate with the survival outcomes and provide additional insights. Our data also demonstrated the predictive ability of the DEM, as it was successfully able to project the survival outcome following aerosolized administration of a novel silver-bearing Ag-PPE-SCK NP antimicrobial formulation to P. aeruginosa infected mice. Lastly, a substantial survival advantage compared with sham treatment was observed in the dose response studies performed using SCC1 and SCC22, compounds with the best collective safety-efficacy profiles. Thus, further investigation of high dose SCC1 and SCC22 as therapeutic options may result in efficacious, yet safe interventions for the treatment of P. aeruginosa infections including pneumonia.
Silver Carbene Complexes (SCCs) and Silver-loaded Polyphosphoester Shell-Crosslinked Knedel-like Nanoparticles (Ag-PPE-SCKs)
The SCCs have been synthesized and characterized as previously described18,19,20,23,26. For preparation of aerosolizable solutions, lipophilic SCCs (SCC23 and SCC28) were first dissolved in DMSO (Sigma Aldrich) and then diluted further in distilled-deionized water (DH2O), whereas the hydrophilic SCCs (SCC1 and SCC22) were first diluted in DH2O, into which DMSO was added. In each sample, the final DMSO concentration was limited to 10% (v/v). PPE-SCK nanoparticles (NPs) were synthesized, loaded with silver, and characterized as previously described31,35. Before testing, the nanoparticles were suspended in sterile DH2O and sonicated for three 15-second pulses at 50% amplitude to achieve complete resuspension (Misonix Microson Ultrasonic Cell Disruptor XL).
Bacterial strains, mammalian cells, and growth conditions
Pseudomonas aeruginosa isolate PA M57-15 was generously donated by Thomas Ferkol, M.D. (Washington University, St. Louis, MO). PA M57-15 was struck from frozen glycerol stocks on to tryptic soy agar plates (Remel) and incubated overnight at 37 °C in a warm room until individual colonies formed. A single colony was inoculated in 10 mL Mueller-Hinton (MH) broth, grown in a shaking incubator (37 °C, 200 rpm) to log phase (OD650 = 0.4), and utilized for experiments after appropriate dilutions. PA M57-15 bacterial suspension at OD650 = 0.4 corresponds to 2–3 × 108 CFU/mL, as verified by repeated serial dilution and plating.
16HBEs (16HBE14o-), generously provided by Dr. D. Gruenert (University of California, San Francisco, CA) are a human bronchial epithelial cell line transformed with SV40 large T-antigen using the replication-defective pSVori plasmid. 16HBEs were used as a model to determine the relative toxicities of the SCCs to airway cells57. Cells between passages 20 to 35 were cultured in Minimum Essential Medium with Earle’s Balanced Salts (Sigma Aldrich) and non-essential amino acids supplemented with penicillin-streptomycin (1%), L-glutamine (1%), and foetal bovine serum (10%). Additionally, primary human dermal fibroblasts (HDFs) were also utilized for in vitro toxicity studies. HDFs at passage 4 were generously donated by Carol Tamminga, M.D. (University of Texas Southwestern Medical Center, Dallas, TX). HDFs were cultured in Dulbecco’s Modified Eagle Medium (Sigma Aldrich) supplemented with penicillin-streptomycin (1%), L-glutamine (1%), and foetal bovine serum (10%) and were utilized between passage 7 to 14 for in vitro toxicity studies. 16HBE and HDF cultures were assessed for bacterial contamination visually, while mycoplasma contamination was assessed both visually and through a PCR-based Universal Mycoplasma Detection Kit assay (ATCC® 30-1012KTM).
Determination of minimum inhibitory and bactericidal concentrations (MICs and MBCs)
The MIC and MBC determinations of the various SCCs and the Ag-PPE-SCK NPs were performed using a standard CLSI protocol with minor modifications. A mucoid clinical isolate of Pseudomonas aeruginosa, PA M57-15, from a cystic fibrosis patient was utilized, because we have previously studied this strain in murine models of P. aeruginosa lung infection21,29,30. PA M57-15 grown to log phase as previously described was diluted to a density of 106 CFU/mL in MH and added 1:1 in a 96-well plate with different concentrations of SCCs dissolved in 95:5 (v:v) DH2O:DMSO solution or the Ag-PPE-SCKs suspended in DH2O. The final SCC concentrations tested were 0.25, 0.5, 0.75, 1, 1.5, and 2 μg/mL and were increased in two-fold increments from 2 μg/mL to 32 μg/mL. The final DMSO concentrations in the wells was 2.5% (v/v) and had no impact on bacterial growth, as determined by growth in the positive control wells. The plates were incubated at 37 °C for 18–24 hours, after which the MIC was determined as the lowest silver concentration that resulted in a lack of growth (clear wells) as determined by visual inspection. Contents of these clear wells were streaked on agar plates and incubated for an additional 24 hours at 37 °C. The MBC was determined as the lowest silver concentration that resulted in no bacterial growth on agar plates. Three technical replicates were employed for each experiment and a total of three biological replicates were performed on separate days (3 technical replicates x 3 biological replicates = 9 total replicates) to account for day-to-day variations in media, bacterial growth, compound dilutions, as well as other experimental conditions. The MIC and MBC values that were identical for at least two readings out of the three are reported.
In vitro LD50 determination by alamarBlue® and calculation of the Drug Efficacy Metric (DEM)
16HBEs and HDFs grown to confluency (90–95%) as described above were sub-cultured, re-suspended in the appropriate medium, and seeded in wells of clear 96-well plate(s) at either 25,000 cells/well (16HBEs) or 15,000 cells/well (HDFs) with 100 µL of feeding media and incubated over 24 hours at 37 °C, 5% CO2, and 100% RH. The cells were then washed once with sterile phosphate buffered saline (PBS, pH = 7.4) and 100 µL of SCCs or the Ag-PPE-SCKs at various concentrations in OPTI-MEM® (Invitrogen) with 3.3% (v/v) DMSO, or without for the Ag-PPE-SCKs, was added to the cells. Next, 10 µL of alamarBlue® (Invitrogen) was added to each well and the plates were re-incubated for 24 h. Finally, the plates were measured for optical density at 570 and 600 nm with a spectrophotometer (POLARstar Omega, BMG Labtech or Cytation 5, BioTek). Untreated cells and media only (with alamarBlue®) were used as controls. Initial testing was performed to ensure that both cell lines were viable in OPTI-MEM® over 24 hours without any adverse effects and the presence of DMSO at the concentrations used in our studies did not affect the cytotoxicity results. The relative viabilities of the cells were determined as per the manufacturer’s instructions and using GraphPad Prism® software to generate a non-linear curve fit and interpolate the in vitro LD50 for each SCC. This assay was performed with three technical replicates for each SCC and Ag-PPE-SCK dose and biological replicates were performed in quadruplicate on separate days (3 technical replicates × 4 biological replicates = 12 total replicates). The DEM for each SCC was determined as the ratio of the molar LD50 and MBC concentrations (LD50/MBC).
Murine P. aeruginosa acute lung infection model
Weight-matched male C57BL/6 J mice aged 6–8 weeks were used for all acute lung infection studies, which were approved by the University of Texas Southwestern Medical Center Institutional Animal Care and Use Committee (IACUC). All experiments were performed in accordance with relevant guidelines and regulations. Animals were housed in a barrier facility under pathogen-free conditions until they were inoculated with bacteria. The previously described clinical mucoid strain of Pseudomonas aeruginosa (PA M57-15) grown to mid-log phase (OD650 = 0.4) in Luria broth (LB) was used for all pulmonary infection experiments. The density of the bacterial culture (CFU/mL) was determined using serial dilution and plating for each experiment.
Mice were anesthetized by intraperitoneal administration of a ketamine (60 mg/kg) and xylazine (8 mg/kg) cocktail, intranasally inoculated using 75 µL of the bacterial inoculum (~1 × 106 CFU per mouse), and assigned randomly into treatment groups. Treatment was administered at 1-hour post-inoculation and again every 12 hours thereafter up to a 5th dose at 49 hours via nebulization of 5 mL of SCC solutions (containing 25 µmol total Ag+ cation per dose for each SCC) or sham treatment. For the head-to-head comparison of unencapsulated SCC1, SCC22, SCC23, and SCC28, all SCCs were dissolved in a 90:10 (v/v) mixture of DH2O and DMSO; whereas, the sham treatment consisted of 90:10 DH2O: DMSO, but with dilute phosphate buffer (1 mM Na2HPO4, 0.2 mM KH2PO4) incorporated to provide tonicity for nebulization. For the dose-response studies with unencapsulated SCC1 and SCC22, 5 mL of SCCs dissolved in DH2O alone or 90:10 (v/v) mixture of DH2O and DMSO was nebulized to provide a total dose of 25, 50, or 100 µmol Ag+ cation per dose for each SCC. Nebulization of the SCCs was achieved using a previously described experimental setup comprising of an Aeroneb Lab apparatus connected to a multi-dosing chamber58. Throughout each study, the mice were monitored constantly and times of death were recorded. Every 24 hours, the mice were weighed and assigned cumulative clinical illness scores (0–6) based on their resting posture (0–2), condition of their fur (0–1), and overall activity level (0–3), with higher scores indicating more severe illness30. The investigators assigning the scores were not blinded to the treatment group, which is a limitation of this study. The survival studies were all performed in duplicate with results pooled.
In vivo efficacy testing of the silver loaded, polyphosphoester, shell-crosslinked, knedel-like nanoparticles (Ag-PPE-SCKs) was carried out in a similar manner as with the SCCs. Ag-PPE-SCKs were suspended in 5 mL DH2O to a concentration of ~5 mM silver, as previously determined by mass spectrometry, and empty PPE-SCKs were suspended corresponding to the same mass of polymer. SCC1, a comparator treatment, was similarly dissolved to 5 mM in 5 mL DH2O, and sham consisted of the DH2O:phosphate buffer solution used in the other studies. The infection model was carried out as before; however, the Ag-PPE-SCKs and PPE-SCKs were dosed at 1 and 25 hours post-infection with the nanoparticles and given sham treatment at 13, 37, and 49 hours. SCC1 and sham treatment groups were dosed at all five time points. Survival studies were performed twice and pooled, though SCC1 was only used in one of the survival studies.
Male C57BL/6 J mice were infected with PA M57-15 and treated with the four SCCs or vehicle as described above. At 25 hours, following three treatments, the mice were humanely euthanized by cervical dislocation following anesthetization by a ketamine/xylazine cocktail. Lungs of the mice were harvested aseptically, the lung sections fixed in 10% formalin for a minimum of 12 hours, and embedded in paraffin using an automated rapid tissue processor (Peloris-Leica Microsystems Inc., Buffalo Grove, IL). Two 5-micron thick sections were obtained from each paraffin block and stained with Haematoxylin/Eosin on an automated stainer (Symphony, Ventana-Roche, Tucson, AZ). Sections were evaluated by light microscopy (Nikon Eclipse-Ni, Nikon Instruments, Inc., Americas), scored using a semi-quantitative scale from 0 (negative), +1 (mild), +2 (moderate), and +3 (severe) for the following parameters: inflammation, consolidation, congestion/haemorrhage, and an aggregate score was calculated for each group59. The presence of bacterial colonies if any was also noted. A pathologist, who was blinded to the treatment received by the mice, performed the examination and analysis of tissues. A total of two mice were used in each treatment group.
All analyses were performed using Prism 6 (GraphPad Software, Inc., San Diego CA), with the exception of Cox proportional hazards regression model, which was performed using R version 3.1.2 (2014 The R Foundation for Statistical Computing, Vienna Austria). A Cox proportional hazards regression model fitted on the survival time (censoring time at 96 h) with treatment as the independent variable was performed to identify the in vitro parameter (MIC, MBC, 16HBE LD50, HDF LD50, 16HBE DEM, or HDF DEM) that demonstrates the highest correlation with survival in vivo. In addition, statistical differences among DEMs were determined using ordinary one-way ANOVA with Tukey’s multiple comparisons test and data were determined to be significantly different for p ≤ 0.05. The in vivo survival curves in the infection model were compared using a Log-rank Mantel-Cox test; whereas, differences in weight change and clinical scores of mice receiving different treatments were analysed using Kruskal-Wallis one-way ANOVA and Dunn’s multiple comparison test.
Antibiotic resistance threats in the United States, 2013. (U.S. Department of Health and Human Services, Centers for Disease Control and Prevention, Atlanta, GA, 2013).
Lyczak, J. B., Cannon, C. L. & Pier, G. B. Lung infections associated with cystic fibrosis. Clin Microbiol Rev 15, 194–222 (2002).
Oliver, A., Canton, R., Campo, P., Baquero, F. & Blazquez, J. High frequency of hypermutable Pseudomonas aeruginosa in cystic fibrosis lung infection. Science 288, 1251–1254 (2000).
Crouch Brewer, S., Wunderink, R. G., Jones, C. B. & Leeper, K. V. Jr. Ventilator-associated pneumonia due to Pseudomonas aeruginosa. Chest 109, 1019–1029 (1996).
Livermore, D. M. Multiple mechanisms of antimicrobial resistance in Pseudomonas aeruginosa: our worst nightmare? Clin Infect Dis 34, 634–640 (2002).
Henwood, C. J., Livermore, D. M., James, D. & Warner, M. Antimicrobial susceptibility of Pseudomonas aeruginosa: results of a UK survey and evaluation of the British Society for Antimicrobial Chemotherapy disc susceptibility test. J Antimicrob Chemother 47, 789–799 (2001).
Hollinger, M. A. Toxicological aspects of topical silver pharmaceuticals. Crit Rev Toxicol 26, 255–260 (1996).
Hostynek, J. J., Hinz, R. S., Lorence, C. R., Price, M. & Guy, R. H. Metals and the skin. Crit Rev Toxicol 23, 171–235 (1993).
Klasen, H. J. A historical review of the use of silver in the treatment of burns. II. Renewed interest for silver. Burns 26, 131–138 (2000).
Klasen, H. J. Historical review of the use of silver in the treatment of burns. I. Early uses. Burns 26, 117–130 (2000).
Silver, S. Bacterial silver resistance: molecular biology and uses and misuses of silver compounds. FEMS Microbiol Rev 27, 341–353 (2003).
Bridges, K., Kidson, A., Lowbury, E. J. & Wilkins, M. D. Gentamicin- and silver-resistant Pseudomonas in a burns unit. Br Med J 1, 446–449 (1979).
Gupta, A., Matsui, K., Lo, J. F. & Silver, S. Molecular basis for resistance to silver cations in Salmonella. Nat Med 5, 183–188 (1999).
McHugh, G. L., Moellering, R. C., Hopkins, C. C. & Swartz, M. N. Salmonella typhimurium resistant to silver nitrate, chloramphenicol, and ampicillin. Lancet 1, 235–240 (1975).
Starodub, M. E. & Trevors, J. T. Silver accumulation and resistance in Escherichia coli R1. J Inorg Biochem 39, 317–325 (1990).
Starodub, M. E. & Trevors, J. T. Mobilization of Escherichia coli R1 silver-resistance plasmid pJT1 by Tn5-Mob into Escherichia coli C600. Biol Met 3, 24–27 (1990).
Lansdown, A. & Williams, A. Bacterial resistance to silver-based antibiotics. Nurs Times 103, 48–49 (2007).
Kascatan-Nebioglu, A. et al. Synthesis from caffeine of a mixed N-heterocyclic carbene-silver acetate complex active against resistant respiratory pathogens. J Med Chem 49, 6811–6818 (2006).
Kascatan-Nebioglu, A., Panzner, M. J., Tessier, C. A., Cannon, C. L. & Youngs, W. J. N-Heterocyclic carbene–silver complexes: A new class of antibiotics. Coord Chem Rev 251, 884–895 (2007).
Hindi, K. M. et al. Synthesis, stability, and antimicrobial studies of electronically tuned silver acetate N-heterocyclic carbenes. J Med Chem 51, 1577–1583 (2008).
Cannon, C. L. et al. In vitro and murine efficacy and toxicity studies of nebulized SCC1, a methylated caffeine-silver(I) complex, for treatment of pulmonary infections. Antimicrob Agents Chemother 53, 3285–3293 (2009).
Hindi, K. M., Panzner, M. J., Tessier, C. A., Cannon, C. L. & Youngs, W. J. The medicinal applications of imidazolium carbene-metal complexes. Chem Rev 109, 3859–3884 (2009).
Panzner, M. J. et al. A theobromine derived silver N-heterocyclic carbene: synthesis, characterization, and antimicrobial efficacy studies on cystic fibrosis relevant pathogens. Dalton Trans 35, 7308–7313 (2009).
Wright, B. D. et al. Synthesis, characterization, and antimicrobial activity of silver carbene complexes derived from 4,5,6,7-tetrachlorobenzimidazole against antibiotic resistant bacteria. Dalton Trans 41, 6500–6506 (2012).
Leid, J. G. et al. In vitro antimicrobial studies of silver carbene complexes: activity of free and nanoparticle carbene formulations against clinical isolates of pathogenic bacteria. J Antimicrob Chemother 67, 138–148 (2012).
Knapp, A. R. et al. Synthesis and antimicrobial studies of silver N-heterocyclic carbene complexes bearing a methyl benzoate substituent. Inorganica Chim Acta 364, 125–131 (2010).
Patton, J. S., Fishburn, C. S. & Weers, J. G. The lungs as a portal of entry for systemic drug delivery. Proc Am Thorac Soc 1, 338–344 (2004).
Meers, P. et al. Biofilm penetration, triggered release and in vivo activity of inhaled liposomal amikacin in chronic Pseudomonas aeruginosa lung infections. J Antimicrob Chemother 61, 859–868 (2008).
Hindi, K. M. et al. The antimicrobial efficacy of sustained release silver-carbene complex-loaded L-tyrosine polyphosphate nanoparticles: characterization, in vitro and in vivo studies. Biomaterials 30, 3771–3779 (2009).
Shah, P. N. et al. Synthesis, characterization, and in vivo efficacy of shell cross-linked nanoparticle formulations carrying silver antimicrobials as aerosolized therapeutics. ACS Nano 7, 4977–4987 (2013).
Zhang, S. et al. Rapid and versatile construction of diverse and functional nanostructures derived from a polyphosphoester-based biomimetic block copolymer system. J Am Chem Soc 134, 18467–18474 (2012).
Lim, Y. H. et al. Preparation and in vitro antimicrobial activity of silver-bearing degradable polymeric nanoparticles of polyphosphoester-block-poly(L-lactide). ACS Nano 9, 1995–2008 (2015).
Muller, P. Y. & Milton, M. N. The determination and interpretation of the therapeutic index in drug development. Nat Rev Drug Discov 11, 751–761 (2012).
Aweda, T. A. et al. The use of 111Ag as a tool for studying biological distribution of silver-based antimicrobials. Med Chem Comm 4, 1015–1017 (2013).
Aweda, T. A. et al. Investigating the pharmacokinetics and biological distribution of silver-loaded polyphosphoester-based nanoparticles using 111Ag as a radiotracer. J Labelled Comp Radiopharm 58 (2015).
Xiao, Q. & Pei, D. High-throughput synthesis and screening of cyclic peptide antibiotics. J Med Chem 50, 3132–3137 (2007).
Zhu, W. L., Hahm, K. S. & Shin, S. Y. Cathelicidin-derived Trp/Pro-rich antimicrobial peptides with lysine peptoid residue (Nlys): therapeutic index and plausible mode of action. J Pept Sci 13, 529–535 (2007).
Lee, D. L. & Hodges, R. S. Structure-activity relationships of de novo designed cyclic antimicrobial peptides based on gramicidin S. Biopolymers 71, 28–48 (2003).
Fjell, C. D., Hiss, J. A., Hancock, R. E. & Schneider, G. Designing antimicrobial peptides: form follows function. Nat Rev Drug Discov 11, 37–5 (2012).
Matsuzaki, K. Control of cell selectivity of antimicrobial peptides. Biochim Biophys Acta 1788, 1687–1692 (2009).
Copple, I. M. et al. Chemical tuning enhances both potency toward nrf2 and in vitro therapeutic index of triterpenoids. Toxicol Sci 140, 462–469 (2014).
Boyce, S. T. & Holder, I. A. Selection of topical antimicrobial agents for cultured skin for burns by combined assessment of cellular cytotoxicity and antimicrobial activity. Plast Reconstr Surg 92, 493–500 (1993).
Hidalgo, E., Bartolome, R. & Dominguez, C. Cytotoxicity mechanisms of sodium hypochlorite in cultured human dermal fibroblasts and its bactericidal effectiveness. Chem Biol Interact 139, 265–282 (2002).
Lineaweaver, W., McMorris, S., Soucy, D. & Howard, R. Cellular and bacterial toxicities of topical antimicrobials. Plast Reconstr Surg 75, 394–396 (1985).
Damour, O. et al. Cytotoxicity evaluation of antiseptics and antibiotics on cultured human fibroblasts and keratinocytes. Burns 18, 479–485 (1992).
Muller, G. & Kramer, A. Biocompatibility index of antiseptic agents by parallel assessment of antimicrobial activity and cellular cytotoxicity. J Antimicrob Chemother 61, 1281–1287 (2008).
Blaser, J. In-vitro model for simultaneous simulation of the serum kinetics of two drugs with different half-lives. J Antimicrob Chemother 15(A), 125–130 (1985).
Firsov, A. A., Vostrov, S. N., Shevchenko, A. A. & Cornaglia, G. Parameters of bacterial killing and regrowth kinetics and antimicrobial effect examined in terms of area under the concentration-time curve relationships: action of ciprofloxacin against Escherichia coli in an in vitro dynamic model. Antimicrob Agents Chemother 41, 1281–1287 (1997).
Firsov, A. A., Vostrov, S. N., Shevchenko, A. A., Portnoy, Y. A. & Zinner, S. H. A new approach to in vitro comparisons of antibiotics in dynamic models: equivalent area under the curve/MIC breakpoints and equiefficient doses of trovafloxacin and ciprofloxacin against bacteria of similar susceptibilities. Antimicrob Agents Chemother 42, 2841–2847 (1998).
MacGowan, A., Rogers, C. & Bowker, K. In vitro models, in vivo models, and pharmacokinetics: what can we learn from in vitro models? Clin Infect Dis 33(3), S214–220 (2001).
Ibricevic, A., Brody, S. L., Youngs, W. J. & Cannon, C. L. ATP7B detoxifies silver in ciliated airway epithelial cells. Toxicol Appl Pharmacol 243, 315–322 (2010).
Bara, A. I. & Barley, E. A. Caffeine for asthma. Cochrane Database Syst Rev, CD001112 (2001).
Bewick, V., Cheek, L. & Ball, J. Statistics review 12: survival analysis. Crit Care 8, 389–394 (2004).
Ruiz, H. K. et al. New amphotericin B-gamma cyclodextrin formulation for topical use with synergistic activity against diverse fungal species and Leishmania spp. Int J Pharm 473, 148–157 (2014).
Spruance, S. L., McKeough, M. B. & Cardinal, J. R. Penetration of guinea pig skin by acyclovir in different vehicles and correlation with the efficacy of topical therapy of experimental cutaneous herpes simplex virus infection. Antimicrob Agents Chemother 25, 10–15 (1984).
Pesanti, E. L. & Nugent, K. M. Modulation of pulmonary clearance of bacteria by antioxidants. Infect Immun 48, 57–61 (1985).
Cozens, A. L. et al. CFTR expression and chloride secretion in polarized immortal human bronchial epithelial cells. Am J Respir Cell Mol Biol 10, 38–47 (1994).
Geller, D. E., Rosenfeld, M., Waltz, D. A., Wilmott, R. W. & AeroDose, T. S. G. Efficiency of pulmonary administration of tobramycin solution for inhalation in cystic fibrosis using an improved drug delivery system. Chest 123, 28–36 (2003).
Knapp, S. et al. Activation of neutrophils and inhibition of the proinflammatory cytokine response by endogenous granulocyte colony-stimulating factor in murine pneumococcal pneumonia. J Infect Dis 189, 1506–1515 (2004).
This work was supported by the Integrated Nanosystems for Diagnosis and Therapy (Program of Excellence in Nanotechnology), HHSN268201000046C from the National Heart, Lung, and Blood Institute (NHLBI) of the National Institutes of Health, by the Welch Foundation (A-0001, KLW), and by departmental support funds for Carolyn L. Cannon, M.D., Ph.D., at the University of Texas Southwestern Medical Center and Texas A&M Health Science Center. The authors thank Thomas Ferkol, M.D. (Washington University, St. Louis, MO) for providing the PA M57-15 isolate of P. aeruginosa and Carol Tamminga, M.D. (University of Texas Southwestern Medical Center, Dallas, TX) for providing the human dermal fibroblasts. The authors also thank the Animal Research Center (ARC) at the University of Texas Southwestern Medical Center for their support with the care and use of the mice used in our infection models.
W.J.Y., M.J.P. and C.L.C. share a patent for silver carbene complexes (SCCs) as antimicrobials. W.J.Y. and M.J.P. have a significant financial interest in the Akron Research Commercialization Corporation that is selling the SCCs described in this research. W.J.Y. and M.J.P. share a patent for encapsulating SCCs in polymeric nanoparticles for uses as chemotherapeutic agents. C.L.C. receives honoraria as a member of a Speaker’s Bureau for Gilead Sciences, manufacturers of the aerosolized antimicrobial, Cayston®. K.L.W., S.Z. and F.Z. share a patent for the synthesis of the polymeric nanosystems described in this manuscript as delivery systems for chemotherapeutic agents.
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Shah, P.N., Shah, K.N., Smolen, J.A. et al. A novel in vitro metric predicts in vivo efficacy of inhaled silver-based antimicrobials in a murine Pseudomonas aeruginosa pneumonia model. Sci Rep 8, 6376 (2018). https://doi.org/10.1038/s41598-018-24200-w