Multidrug-resistant bacterial strains are a rapidly emerging healthcare threat; therefore it is critical to develop new therapies to combat these organisms. Prior antibacterial strategies directly target pathogen growth or viability. Host-directed strategies to increase antimicrobial defenses may be an effective alternative to antibiotics and reduce development of resistant strains. In this study, we demonstrated the efficacy of a pyrimidine synthesis inhibitor, N-phosphonacetyl-l-aspartate (PALA), to enhance clearance of methicillin-resistant Staphylococcus aureus (MRSA), Pseudomonas aeruginosa, and Acinetobacter baumannii strains by primary human dermal fibroblasts in vitro. PALA did not have a direct bactericidal effect, but enhanced cellular secretion of the antimicrobial peptides human β-defensin 2 (HBD2) and HBD3 from fibroblasts. When tested in porcine and human skin explant models, a topical PALA formulation was efficacious to enhance MRSA, P. aeruginosa, and A. baumannii clearance. Topical PALA treatment of human skin explants also resulted in increased HBD2 and cathelicidin (LL-37) production. The antimicrobial actions of PALA required expression of nucleotide-binding, oligomerization domain 2 (NOD2), receptor-interacting serine/threonine-protein kinase 2 (RIP2), and carbamoyl phosphatase synthase II/aspartate transcarbamylase/dihydroorotase (CAD). Our results indicate that PALA may be a new option to combat multidrug-resistant bacterial infections of the skin through enhancement of an integral pathway of the cutaneous innate immune defense system.
A major healthcare problem is the rapidly expanding prevalence of multidrug-resistant (MDR) bacterial strains1. Over 2 million people in the United States acquire serious infections with MDR strains each year, and approximately 23,000 individuals die from these infections2. The loss of effective antimicrobial treatments has significant impact on routine medical care; common infections now often require more toxic, expensive, and less efficacious antibiotics. This significantly affects not only vulnerable populations, such as immune comprised individuals, the elderly, infants, and those with diabetes or other chronic health conditions, but also healthy individuals undergoing surgical procedures that require effective protection against secondary infection. With the alarming increase in antibiotic resistance, there is an unmet clinical need to design novel and innovative methods to treat MDR bacterial infections.
Skin is frequently colonized with polymicrobial populations that belong to the ESKAPE family, including Enterococcus faecium, Staphylococcus aureus, Klebsiella pneumoniae, Acinetobacter baumannii, Pseudomonas aeruginosa and Enterobacter spp3,4. These organisms are opportunistic pathogens and are the leading cause of nosocomial infections2,5. ESKAPE pathogens are characterized by a high rate of antimicrobial resistance that is acquired through multiple mechanisms that include: drug inactivation, modification of drug binding sites, increased drug efflux, and enhanced biofilm formation5. These pathogens often cause a local infection through a breach in the skin. Even in otherwise healthy children and adults, many of these cases progress to fatal, invasive infections or severe, life-threatening conditions, such as necrotizing fasciitis, pneumonia, septicemia, and endocarditis.
Skin is the first line of defense in the human body against invading pathogens6. It presents both a physical and chemical barrier to invasion through the presence of a hydrophobic stratum corneum and the constitutive expression of several classes of antimicrobial peptides (AMPs), such as cathelicidin and β-defensins7. When this barrier is breached due to wounds, cuts, or abrasions, cells present in the skin epidermis and dermis play important roles in amplifying protective defenses and generating specific immune responses8,9,10. Pattern recognition receptors, like Toll-like receptors (TLRs) and NOD-like receptors (NLRs), are key components of the innate immune response that sense the infection and initiate signaling that result in the secretion of chemokines, cytokines, and AMPs11. These secreted products act to provide immediate antimicrobial activity, activate resident cells, and recruit additional immune cells to clear the infection12,13. There is increasing interest in augmenting or enhancing these innate immune responses to prevent or treat bacterial infections, as this strategy would not further contribute to the rise of MDR strains and could potentially be combined with other antimicrobial therapies14,15.
In a previous study, we identified a small molecule compound that enhances the antimicrobial activity of the pattern recognition receptor, nucleotide-binding, oligomerization domain 2 (NOD2)16. NOD2 is an intracellular sensor of both intracellular and extracellular bacterial pathogens, including Salmonella, S. aureus, A. baumannii, and P. aeruginosa17,18,19. It is expressed in both immune cells and barrier cells of the skin20, where it plays critical roles in wound healing and cutaneous defense against pathogens19,21. Mice deficient in NOD2 expression (Nod2−/−) have delayed wound healing due to defective keratinocyte migration and reduced neutrophil recruitment21. Additionally, Nod2−/− mice infected subcutaneously with S. aureus have impaired bacterial clearance and an exacerbated ulcerative response19. NOD2 functions in keratinocytes to regulate the expression of AMPs, such as human β-defensin 2 (HBD2) and HBD3, through the activation of an intracellular signaling cascade that requires receptor-interacting serine/threonine-protein kinase 2 (RIP2)15,22,23. One challenge to modulating the activity of this pathway is that the NOD2 protein does not have a specific, pharmacologically targetable enzyme activity. However, we identified that NOD2 activity is negatively regulated by the enzyme carbamoyl phosphatase synthase II/aspartate transcarbamylase/dihydroorotase (CAD)16,24. CAD is an enzyme required for de novo pyrimidine synthesis and can be inhibited by a specific small molecule compound N-phosphonacetyl-l-aspartate (PALA)25. Our studies in intestinal epithelial cells demonstrated that PALA treatment specifically relieves CAD-mediated repression of NOD2 activity, resulting in enhanced clearance of intracellular bacteria16. The current study tests whether this method of NOD2 activation to stimulate innate immune responses could be an effective approach to target antibiotic resistant bacterial infections in skin wounds.
The results of this study show that PALA enhances bacterial clearance in a NOD2 signaling pathway-dependent manner using in vitro models. These infection models include studies of primary human dermal fibroblasts, as well as ex vivo pig and human skin explants. Results demonstrate that PALA is not directly bactericidal or cytotoxic. Instead, PALA relieves the CAD-mediated inhibition of NOD2 signaling to result in enhanced secretion of antimicrobial peptides that are effective in killing both Gram-positive and Gram-negative bacteria of the ESKAPE pathogen family. Our results indicate that PALA may be a new option to combat multidrug-resistant bacterial infections of the skin through enhancement of an integral pathway of the cutaneous innate immune defense system.
PALA is not directly bactericidal, but enhances bactericidal activity of normal human dermal fibroblasts (NHDF)
Several pattern recognition receptors including NOD2 are expressed in skin and contribute to host defenses against S. aureus19. Therefore, we examined whether PALA treatment is effective in generating antimicrobial responses against methicillin-resistant S. aureus (MRSA) in primary fibroblasts derived from human skin (Fig. 1). NHDF were treated with up to 25 µM PALA for 16 hours, and then infected with a bioluminescent MRSA strain26, followed by quantification of colony forming units (cfu). MRSA viability was dose-dependently decreased by PALA treatment of NHDF cultures, with significant differences observed at concentrations of 5, 10, and 25 µM (Fig. 1a). The kinetics of bacterial clearance in NHDF cultures was measured by quantification of MRSA bioluminescence over time in the presence and absence of PALA. NHDF were pre-treated with 25 µM PALA for 60 minutes, then infected with bioluminescent MRSA, and bioluminescence monitored over 120 minutes. PALA-mediated enhancement of MRSA clearance was observed within 60 minutes and was maintained at 90 and 120 minutes (Fig. 1b). These results demonstrate that PALA decreases MRSA viability rapidly and in a dose-dependent manner.
PALA inhibits the aspartate transcarbamylase (ATC) activity of CAD to prevent de novo pyrimidine synthesis25. Bacteria also express ATC; therefore, we investigated whether the decreased MRSA cfu observed after PALA treatment is due to direct bactericidal or bacteriostatic effects (Fig. 1c). Early log-phase cultures of bioluminescent MRSA were supplemented with either PALA (250 µM) or gentamycin (50 µg/ml) and growth monitored over 120 minutes. MRSA grown in unsupplemented broth and PALA supplemented cultures showed similar increases in bioluminescent signal, indicating robust bacterial growth (Fig. 1c). In contrast, cultures supplemented with the antibiotic gentamycin did not grow. These results indicate that PALA, even at doses 10-times higher than an effective concentration to induce a cellular antimicrobial response, does not have direct bactericidal or bacteriostatic activity.
PALA is not cytotoxic and does not inhibit wound healing responses in NHDF
One concern about the therapeutic use of a pyrimidine synthesis inhibitor, such as PALA, is the potential for cytotoxic effects on host cells. To determine the cytotoxicity of PALA, NHDF cells were exposed to a range of PALA concentrations shown to induce an antibacterial effect (0–25 µM) for 24 hours and cell viability determined using the lactate dehydrogenase (LDH) release assay. No change in cell viability was observed at the highest concentration of PALA tested (25 µM), a dose that is most effective in clearing bacteria from the cells (Fig. 2a). The impact of PALA on cellular proliferation was also measured by an XTT cell proliferation assay. No difference in cellular growth was observed between untreated and PALA (25 µM) treated NHDF after 24 hours (Fig. 2b). Additionally, the effects of PALA on NHDF cell migration were assessed by live cell imaging of in vitro scratch wound assays to determine if PALA may inhibit wound healing responses. No significant differences in cell migration were observed between untreated and PALA-treated NHDF over the 27 hour time course (Fig. 2c,d; Supplemental Movies S1 and S2). These findings indicate that PALA rapidly induces an antibacterial response to MDR bacterial infection at a non-cytotoxic concentration in primary human skin-derived cells.
PALA treatment results in clearance of ESKAPE pathogens and production of broad-spectrum AMPs by NHDF
In order to characterize the spectrum of antibacterial activity induced by PALA in NHDF, we tested the bactericidal activity of conditioned supernatants on both Gram-positive and Gram-negative bacterial strains of the ESKAPE pathogen family. Mid-log cultures of MRSA, P. aeruginosa, and A. baumannii were supplemented with conditioned supernatants from NHDF treated with or without PALA and bacterial viability measured by selective plating. Supernatants from PALA treated cells were effective in reducing recovered cfu of all three strains (Fig. 3a), indicating that PALA stimulates the secretion of broad spectrum antimicrobial factors from NHDF.
The major families of AMPs expressed in the skin and induced by bacterial infection are cathelicidins (LL-37) and β-defensins (HBD2 and HBD3)7. Therefore, we quantified the levels of these candidate AMPs released into the media from untreated or PALA treated NHDF by ELISA. The protein levels of HBD2 and HBD3, were found to be significantly elevated in supernatants from PALA treated cells, while secreted LL-37 levels were unaffected (Fig. 3b). Further analysis of PALA treated NHDF was performed to determine whether PALA treatment induces transcriptional upregulation of AMPs or primarily stimulates AMP secretion. Transcript levels of DEFB4A (HBD2), DEFB103B (HBD3), and CAMP (cathelicidin) in PALA-stimulated NHDF were quantitated relative to levels in unstimulated cells by qRT-PCR. PALA stimulated the transcription of the genes encoding HBD2 and cathelicidin, but not HBD3 (Fig. 3c). These results demonstrate that in NHDF, PALA primes the production of cathelicidin, increases the release of HBD3, and upregulates both the production and release of HBD2, resulting in an enhanced ability of NHDF to kill both Gram-positive and Gram-negative ESKAPE pathogens.
Topical application of PALA enhances the clearance of MRSA, P. aeruginosa and A. baumannii from skin explants
In order to translate our findings into a more clinically-relevant context, a topical formulation of PALA was prepared and tested for induction of antibacterial activity in primary skin explants (Fig. 4). Biopsies from fresh skin samples obtained from Yorkshire pigs were maintained ex vivo in an air-liquid interface culture and tested within 24 hours of collection. Explants were wounded with a 25 g needle and infected with MRSA for 1 h. Infected biopsies were then treated topically with either Aquaphor (vehicle control), 2% (w/w) PALA, or the triple antibiotic ointment Neosporin for 4 hours. Bacterial load was determined by selective plating of biopsy homogenates. Significantly fewer cfu were recovered from biopsies treated with 2% PALA or Neosporin, as compared to the Aquaphor treated group (Fig. 4a). A similar effect was observed when topical PALA was tested on ex vivo human skin explants, where treatment with 2% PALA was significantly more effective in killing bacteria as compared to Aquaphor treated biopsies after 4 hours (Fig. 4b). Excitingly, in addition to MRSA, 2% PALA treatment (24 hours) improved clearance of P. aeruginosa and A. baumannii by human skin explants (Fig. 4c,d and e). The results indicate that topical application of PALA effectively stimulates an antibacterial response against three different members of the ESKAPE pathogen family in skin samples that results in enhanced bacterial clearance.
Topical application of PALA enhances AMP production in human skin explants
We quantified the levels of candidate AMPs (HBD2, HBD3, and LL-37) in human skin explants treated with Aquaphor, 2% PALA, or Neosporin by ELISA of tissue homogenates. The protein levels of HBD2 and LL-37 were significantly elevated in explants treated with 2% PALA compared to the control (Aquaphor), with no significant differences observed in the HBD3 levels across various treatment groups (Fig. 5a,c and e). HBD2 levels were also significantly elevated by Neosporin treatment as compared to Aquaphor treatment (Fig. 5a). Immunohistochemistry was performed on MRSA infected skin explants to visually detect the level and location of AMP expression in response to topical PALA treatment (Fig. 5b,d,f). Similar to the ELISA results, HBD2 and LL-37 staining was more intense in explants treated with 2% PALA in comparison to Aquaphor, while HBD3 staining was equivalent between treatment groups. HBD2 expression primarily co-localized to the differentiating keratinocyte layers and not the stratum basale (Fig. 5b). HBD3 staining localized throughout the epidermis, and did not change in response to 2% PALA treatment (Fig. 5d). Cathelicidin (LL-37) staining in Aquaphor treated explants was most pronounced in the stratum corneum and stratum lucidum (Fig. 5f). After PALA treatment, LL-37 was detected more widely in the epidermis to include the lucidum, granular, and spinosum layers (Fig. 5f). These results indicate that topical PALA treatment of skin explants enhances the production of HBD2 and LL-37 with broad-spectrum activity, which is effective in killing three different pathogens.
PALA treatment specifically increases NOD2-dependent S. aureus clearance
NOD1 and NOD2 are intracellular NLR proteins reported to sense and respond to extracellular pathogens, such as S. aureus19,27,28. We confirmed that NOD1 and NOD2 can sense S. aureus using a combination of luciferase reporter assays and bacterial clearance assays in HEK293T cells (Fig. 6). HEK293T cells do not express NLRs or TLRs endogenously and allow for the study of individual pattern recognition receptor responses when expressed exogenously. HEK293T cells were transfected with empty expression vector, NOD1, or NOD2 expression plasmids, as well as an NFκB-dependent luciferase reporter construct and a constitutive β-galactosidase expression transfection efficiency control. The cells were subsequently infected with S. aureus, followed by assessment of NLR-dependent NFκB signaling and antibacterial clearance. Vector transfected cells did not increase NFκB activity in response to S. aureus infection, indicating they lacked expression of pattern recognition receptors required to sense this bacterium (Fig. 6a). Exogenous expression of NOD1 or NOD2 resulted in a robust S. aureus-induced NFκB activation. These data confirm that both NOD1 and NOD2 are sensors of extracellular S. aureus and activate downstream signaling pathways in response to S. aureus infection.
Previously, we demonstrated that PALA enhanced the clearance of the intracellular pathogen Salmonella in a NOD2-dependent manner16. We tested whether PALA also requires NOD2 expression to stimulate the release of antimicrobial factors that target extracellular pathogens, such as S. aureus. HEK293T cells were transfected with NOD1 or NOD2 expression plasmids. The transfected cells were treated with or without PALA for 24 hours, and the bactericidal effect of conditioned supernatants was tested on S. aureus cultures. NOD2 expression was required for PALA treatment to increase secreted antibacterial activity, as only supernatants from NOD2 expressing cells demonstrated enhanced S. aureus killing in response to PALA treatment (Fig. 6b). These experiments confirm that both NOD1 and NOD2 can sense extracellular pathogens, like S. aureus, and demonstrate that PALA treatment increases secretion of antibacterial factors that increase bacterial clearance of these organisms in a NOD2-dependent manner.
The antibacterial effects of PALA require expression of CAD and NOD2 signaling molecules
Pharmacologic inhibitors often have off-target effects; therefore, we determined the requirement for CAD expression for the antimicrobial effects of PALA stimulation. NHDF were transfected with non-targeting (shControl) and CAD-targeting (shCAD) shRNA constructs and CAD protein levels were determined by immunoblot to confirm RNAi-mediated knockdown of CAD expression (Fig. 7a). Transfected cells were treated with or without PALA for 24 hours and conditioned supernatants added to mid-log phase MRSA cultures to determine bactericidal activity by selective plating. PALA-stimulated antimicrobial activity observed in shControl conditioned supernatants was lost in supernatants from shCAD cells (Fig. 7b). These results indicate that PALA requires CAD expression to induce an antimicrobial response in NHDF.
Next, we investigated whether components of the NOD2 signaling cascade were required for PALA enhanced clearance of MRSA by NHDF. NOD2 signaling requires RIP2, a dual specificity kinase, to activate a signal transduction cascade in response to bacterial infection15. NHDF were transfected with shRNA targeting NOD2 (shNOD2), RIP2 (shRIP2), or a non-targeting control (shControl) plasmid and knockdown was confirmed by qRT-PCR or immunoblot (Fig. 7c,d). Transfected cells were subsequently treated with or without PALA for 24 hours and bactericidal activity of the conditioned supernatants assessed on mid-log phase MRSA cultures. PALA treatment of shControl transfected NHDF increased the bactericidal activity of conditioned supernatants (Fig. 7e). In contrast, knockdown of NOD2 or RIP2 resulted in similar levels of bacterial killing between supernatants from untreated and PALA treated cells. Knockdown of NOD2 or RIP2 also impaired the secretion of HBD2 and HBD3 from these cells as determined by ELISA of conditioned supernatants used for bacterial clearance assays (Fig. 7f,g). These results indicate NOD2 and RIP2 expression are required for the antibacterial effects of PALA treatment in NHDF and suggests that NOD2 signaling plays an important role in this response.
Multiple factors have contributed to the rise of MDR pathogens, including the misuse and overuse of antibiotics, supplementation of agricultural feed with antibiotics, the rapid cross-transfer of antibiotic resistance genes between bacteria, as well as a decreased level of antibiotic development in pharmaceutical company pipelines29,30. As a result, it is predicted that there will be 300 million premature deaths worldwide due to antimicrobial resistance by 2050 if there is not a dramatic change to our approach to MDR pathogens31. In this scenario, deaths from infectious disease are estimated to be 10 million/year, exceeding cancer-related mortality and making it one of the leading causes of death31. To avoid this, it will require a multi-faceted approach to infection control that integrates not only additional antibiotics, but also improved infection prevention measures, increased awareness and understanding of MDR, greater education regarding optimal application of antibiotic therapy, and accelerated development of novel antimicrobial agents. This study identifies a small molecule agent, PALA, as new potential addition to the arsenal to combat MDR bacterial infections.
An ever increasing number of studies demonstrate the benefits of stimulating pattern recognition receptors to protect against microbial infection through induction of a broad spectrum antimicrobial response29,32,33. One example of this is the administration of flagellin to stimulate TLR5-mediated immune responses, which provided protection against P. aeruginosa in a lung infection model34. However, one danger of this approach is the potential to exacerbate inflammation and tissue damage through overstimulation of an inflammatory immune response. This was observed in initial studies with TLR4 agonists that included a toxic lipid A component of endotoxin; use of more selective monophosphoryl lipid A (MPLA) or aminoalkyl gluosaminide phosphates (AGPs) are now clinically in use as vaccine adjuvants33. Our results indicate that PALA acts to increase basal NOD2 signaling activity by inactivating CAD, a negative regulator of NOD2 (Fig. 7)16. Our data also demonstrate that derepression of NOD2 by PALA resulted in increased expression and release of AMPs (Figs 3b,c and 7f,g), while not inducing the release of the pro-inflammatory cytokines IL-1β, IL-6, or TNFα from NHDF (data not shown). While the molecular mechanisms underlying this differential enhancement of NOD2-dependent responses requires further study, this feature of PALA to boost antimicrobial factor production, rather than directly stimulate inflammatory immune responses may increase the specificity and safety of this approach to infection control.
NOD2 is an integral component of the innate immune system and serves as sensor for a wide range of intracellular and extracellular bacteria11,15. Studies in Nod2−/− mice have shown the importance of NOD2 in maintaining antimicrobial homeostasis in the skin, as well as promoting wound healing responses. Nod2−/− mice are more susceptible to subcutaneous infection with S. aureus and develop an exacerbated ulcerative response27. Additionally, mice deficient in NOD2 expression are impaired in acute wound healing due to a combination of altered skin microbiota35, delayed immune cell recruitment to wound sites21, and impaired epidermal proliferation and migration21. With the key role of NOD2 in mitigating bacterial proliferation in skin wounds and impacting the wound-healing cascade, it is definitely a therapeutic target of interest to address the problem of MDR infection.
There are several challenges to targeting NOD2 therapeutically, safely, and specifically. Stimulation of NOD2 responses by its ligand, muramyl dipeptide (MDP), has been demonstrated to induce broad-spectrum immune responses in mice that are protective against both bacterial and viral infections15,36. However, in humans, MDP has enhanced toxic, pyrogenic, and arthritogenic properties, precluding its use therapeutically37. This has led to the development of non-toxic MDP derivatives that retain select immunostimulatory activities, which are demonstrating benefit as an antiviral therapy in early stage clinical trials38,39. In our studies, there were no detected toxic effects of PALA on cellular viability, proliferation, or migration of primary human cells at concentrations that were found to be immunomodulatory (Fig. 2; Supplementary Movies 1 and 2). Additionally, we are targeting the NOD2 pathway with a small molecule compound, rather than a bacterial cell wall component that may be sensed by additional NLRs, such as NLRP315. The compound PALA is a rationally-designed, transition-state inhibitor of the ATCase activity of CAD25, making it extremely specific to targeting this enzyme. The specificity of PALA to induce an antibacterial response through binding CAD was confirmed in this study (Fig. 7a) and in our previous study16 through RNAi-mediated knockdown of CAD. Interestingly, RNAi-mediated CAD knockdown blocked PALA-enhanced bactericidal activity, but it was not sufficient to induce the same level of AMP secretion from NHDF (Supplementary Fig. S1) or enhance the bactericidal activity of conditioned supernatants to the same degree as PALA treatment (Fig. 7b). These results may indicate that either the CAD knockdown was not efficient enough to induce as strong of a response as PALA treatment, or that the underlying molecular mechanisms involved are complex (i.e. differential requirements of CAD protein expression for NOD2 subcellular localization to activate the antibacterial response and CAD enzyme activity to repress NOD2 activity).
Newer therapeutic approaches to MDR infections are focused on aspects of host-pathogen interaction, rather than solely targeting bacterial viability. These approaches include targeting mechanisms involved in pathogen virulence, such as neutralization of bacterial toxins, prevention of biofilm formation or altering bacterial genes to “disarm” or disable the bacteria, rather than killing them29. For example, antibodies targeting S. aureus α-toxin, an important mediator of MRSA virulence, increased survival of mice challenged with a range of clinical S. aureus isolates in a pneumonia model40 and one antibody (AR301/Aridis) has already completed testing in Phase I/II human clinical trials41. Another promising approach targets quorum-sensing to impair the production of bacterial virulence factors, which has shown efficacy in a pre-clinical model of MRSA wound infection42. By disarming pathogens, these approaches make bacteria more sensitive to antibiotics and combination therapy results in synergistic effects, even on bacteria that are resistant to antibiotic monotherapy42. Interestingly, studies with MDP-derivatives have also demonstrated a synergistic effect with antibiotics, such as cefmenoxime, to clear infections with Klebsiella pneumonia43. As PALA does not have direct bactericidal effects (Fig. 1c), but rather mediates its effects through NOD2 signaling (Fig. 7e–g); it is anticipated that its antibacterial activity could also synergize with other antimicrobial agents that directly target bacteria (i.e. antibiotics, silver compounds, etc.), increasing their utility in MDR infections.
Exogenous application of small cationic peptides like cathelicidin and defensins, also known as “natural antibiotics” have also been shown to be efficacious in various infection models14. This is highlighted by studies examining the role of cathelicidin in control of bacterial infection and colonization. Cnlp-null (cathelicidin-deficient) mice demonstrated decreased clearance of group A Streptococcus44, while increased colonization of S. epidermidis was observed in a porcine wound model after inhibition of the active form of cathelicidin by neutrophil elastase cleavage45. Due to their important role in antimicrobial defense, pathogenic bacteria have evolved multiple mechanisms to decrease host production or activity of AMPs46. This has led to additional immune targeting therapeutic approaches to counteract pathogen-induced downregulation of AMPs and preserve host defenses47,48. This approach is now being studied in clinical trials, with a Phase II trial underway testing the efficacy of vitamin D supplementation on MRSA colonization49 and a successful Phase II trial reported for the treatment of shigellosis with sodium butyrate47,50. Recent studies have also focused on targeting S. aureus infections using various synthetic antimicrobial peptides51,52 and some of these peptides were shown to be effective against biofilms52. The results of our study also demonstrate the induction of an antibacterial response that targets multiple members of the ESKAPE pathogen family by PALA in both NHDFs and skin explants (Figs 3 and 4). Keratinocytes comprising the skin epidermis express HBD1-4. Of the four beta-defensins, HBD-1 is constitutively expressed in the skin and HBD2/HBD3 are released in response to bacterial infection53. On the other hand, cathelicidin (LL-37) is expressed by multiple cell types including neutrophils, mast cells, eccrine glands and keratinocytes as its inactive form hCAP 1853,54. In human skin, hCAP 18 is processed to form LL-37 by stratum corneum enzymes and proteases and is inducible by wounding and inflammation53,55. hCAP 18/LL-37 has been shown to be predominantly present in the granular and spinous layer of the epidermis53,54. AMPs exhibit broad spectrum antimicrobial activity and also possess the ability to modulate the host immune response. In this study we observed an increase in the production of both HBD2 and LL-37 protein upon infection of skin explants with MRSA and PALA treatment (Fig. 5) with no significant differences observed in HBD3 protein production. This result was consistent with the upregulation in genes encoding HBD2 and LL-37 observed in NHDF cells upon PALA treatment (Fig. 3c). While LL-37 levels were significantly increased in the human skin explant model in the differentiating keratinocyte layers of the skin, we observed no differences in LL-37 production in the conditioned media from fibroblasts (Fig. 3b). This may be due to technical difficulties in detecting secreted LL-37 in vitro, as another study was only able to detect LL-37 protein produced by cultured keratinocytes after immunoprecipitation of whole cell extracts; the levels in conditioned media were not detectable54. This was attributed to degradation of LL-37 upon secretion, presence of LL-37 binding proteins, or protease inhibitors in the media that interfered with production of mature LL-3754. Additionally, cell type response differences, cross-talk between various cell types in the skin epidermis8, or the complexity of the cytokine/chemokine milieu in response to infection all possibly contribute to the differences we observe between our in vitro fibroblast cultures and human skin explant model. The enhanced antibacterial defense in this study is potentially mediated, at least in part, through increased production of AMPs (Figs 3 and 5). Therefore, we predict that in vivo PALA treatment may act to maintain expression of AMPs during infection to promote bacterial clearance, rather than enhance inflammation.
To summarize, this study demonstrated that the pyrimidine synthesis inhibitor, PALA, derepresses the NOD2 signaling pathway and enhances antimicrobial, innate immune responses in human in vitro and ex vivo skin systems to increase clearance of ESKAPE pathogens. This approach could potentially be used alone or as adjunctive therapy to increase the efficacy of other antimicrobial treatments and help patients with wounds infected with bacterial strains non-responsive to traditional antibiotic treatments. This strategy to target antibiotic resistant bacteria through priming of the innate immune response is an important step towards designing new strategies to kill bacteria without increasing the burden of antibiotic resistance.
Reagents, Antibodies, and Plasmids
N-phosphonacetyl-l-aspartate (PALA, NSC224131) was obtained from the National Cancer Institute (NCI)/Division of Cancer Treatment and Diagnosis (DCTD)/Developmental Therapeutics Program (DTP) Open Chemical Repository (http:dtp.cancer.gov). Aquaphor® and Neosporin® were purchased from Target (Cleveland Heights, OH). Gentamycin solution was purchased from Sigma (St. Louis, MO). Rabbit monoclonal anti-CAD antibody (EP711Y) was purchased from Novus Biologicals (Littleton, CO). Rabbit polyclonal anti-RICK (H-300) was purchased from Santa Cruz Biotechnology (Santa Cruz, CA). Rabbit monoclonal anti-GAPDH (14C10) was purchased from Cell Signaling Technologies (Danvers, MA). Mouse monoclonal anti-α-tubulin (T5168) was purchased from Sigma. Antibodies against LL-37 (sc-166770) and HBD2 (sc-20798) were purchased from Santa Cruz Biotechnology. Anti-HBD3 antibody was purchased from Novus Biologicals (NB200-117). The plasmids, pcDNA3-HA-NOD1, pcDNA3-HA-NOD2, pBVIII-Luc, and pCMV-βgal were gifts of Gabriel Nuñez (University of Michigan) and have been previously described56. MISSION short hairpin RNA (shRNA) constructs targeting CAD (NM_004341.3-6910s21c1), NOD2 (NM_022162.1-2959s1c1), RIP2 (NM_003821.5-2364s21c1), and non-targeting shRNA control (SHC002) were purchased from Sigma.
S. aureus Reynolds capsular serotype 5 (CP5)57 was a gift of Michelle Longworth (Cleveland Clinic). The clinically-derived, community-acquired, methicillin-resistant S. aureus (MRSA) strain MW2 (SAP227)26 with a stable chromosomal integration of the lux operon from Photorhabdus luminescens, was a gift of Roger Plaut (FDA). P. aeruginosa GFP (ATCC 10145GFP) and A. baumanni 5377 (ATCC 17978) strains were purchased from the American Type Culture Collection (ATCC; Manassas, VA). S. aureus and A. baumanni strains were grown in Tryptic Soy Broth (TSB) at 37 °C with aeration. P. aeruginosa was grown in Luria Bertani (LB) broth at 37 °C with aeration. Mid-log phase cultures were prepared by growing 1:7 dilutions of overnight cultures for 90 minutes at 37 °C with aeration.
The human embryonic kidney 293-HEK293T/17 (CRL-11268) cell line was purchased from ATCC and cultured in Dulbecco’s Modified Eagle Medium (DMEM) supplemented with 10% fetal bovine serum (FBS; Life Sciences, Carlsbad, CA). Normal adult human dermal fibroblasts (NHDF; CC-2511) were purchased from Lonza (Allendale, NJ) and cultured in FGM-2 media (CC-3132; Lonza). NHDF were transfected with shRNA contructs using a Nucleofector (Lonza) and the dermal fibroblast transfection kit (VPD-1001) according to manufacturer’s recommendations and assayed 48 h post-transfection. HEK293T/17 cells were transfected with expression constructs using Polyfect (Qiagen, Valencia, CA) according to manufacturer’s instructions and treated with 25 µM PALA 48 h post-transfection for collection of conditioned supernatants for bactericidal assays. Cell viability was determined by 2,3-Bis-(2-Methoxy-4-Nitro-5-Sulfophenyl)-2H-Tetrazolium-5-Carboxanilide (XTT) assay (Roche, Indianapolis, IN) and lactate dehydrogenase (LDH) secretion (Fisher Scientific, Waltham, MA) according to manufacturer’s instructions.
In Vitro Scratch Wound Assay
NHDF were plated in removable culture 2 well inserts (ibidi; Munich, Germany) at 24,000 cells/insert well in triplicate. After 24 hours, the inserts were removed and fresh media added with or without 25 µM PALA. Automated time-lapse microscopy was performed using a Leica DMI6000 inverted microscope with LAS X software (Leica Microsystems, GmbH; Wetzlar, Germany) and images captured every 15 minutes for 27 hours by a Hamamatsu Orca Flash4 camera (Hamamatsu Photonics; Shizuoka, Japan). Image analysis was performed using a custom macro in ImagePro Plus software (Media Cybernetics; Rockville, MD).
NHDF cells treated with or without 25 μM PALA in triplicate for 16 hours were collected and RNA isolated using the Qiagen RNeasy Mini Kit. RNA was converted to cDNA using the BioRad iScript cDNA synthesis kit. qPCR was performed in duplicate using SYBR Green supermix and quantified using the 2−ΔΔCT method58. Primers targeting DEFB4A (HBD2), DEF103B (HBD3), CAMP (cathelicidin), and NOD2 are listed in Supplementary Table S1.
Luciferase Reporter Assays
HEK293T/17 cells were plated at 10,000 cells/well in 48 well plates in triplicate for transfection using Polyfect (Qiagen) according to manufacturer’s protocol. Transfected cells were infected 24 hours post-transfection with S. aureus CP5 at a multiplicity of infection (MOI) of 5 for 6 hours. Cells were collected in 1× reporter lysis buffer (100 µL/well; Promega, Madison, WI) and subjected to two freeze/thaw cycles. Luciferase and β-galactosidase activity measured as previously described59 and presented as luciferase activity normalized to transfection efficiency determined by β-galactosidase levels.
Cells were washed 2× in PBS, then lysed in Ginger buffer (310 mM Tris pH 6.8, 25% glycerol, 5% SDS, 715 mM 2-mercaptoethanol, 125 mg/mL bromphenol blue) on ice for 10 minutes. The resulting lysate was separated by SDS-PAGE and proteins transferred to a polyvinylidene fluoride membrane using the iBlot2 system (ThermoFisher Scientific; Cleveland, OH). Membranes were blocked in 5% milk/TBST (Tris buffered saline, 0.1% Tween-20) and then probed with primary antibodies overnight at 4 °C. After washing with TBST, blots were probed with horseradish peroxidase-conjugated secondary antibodies for 1 h in 2.5% milk/TBST. Blots were developed by enhanced chemiluminescence. Uncropped scans of immunoblots used to create Fig. 7 are included in Supplementary Fig. S2.
NHDF were seeded at 20,000 cells/well in duplicate in 24 well plates in FGM-2 media the day before treatment. Media was changed to DMEM + 10% FBS and stimulated with PALA (1–25 µM) for 1 h prior to infection with SAP227 (MOI = 5) for 2 hours. Bioluminescence of SAP227 was monitored at 30 minute intervals for 10 s/well in a Flexstation 3 (Molecular Probes, Eugene; OR). After 2 h, supernatants were collected and cells lysed in 50 µL 1%Triton X-100/PBS on ice for 10 minutes. Cell lysates and supernatants were combined and viable bacteria determined through serial dilution and plating of duplicate samples on LB agar plates.
NHDF Conditioned Supernatant Bactericidal Activity Assays
NHDF were plated at 20,000 cells/well in 24 well plates in FGM-2 media. The next day, the media was changed to DMEM + 10% FBS and cells were stimulated with PALA (1–25 µM) for 16 hours. Cell supernatants were collected and cell debris was removed by centrifugation (500xg, 5 minutes). Antibacterial activity was assessed in triplicate by combining 50 µL of conditioned media with 100,000 cfu for 1–2 h in a total volume of 100 µL. Bacterial viability was determined through serial dilution and the plating of duplicate samples on LB agar plates. AMP levels in conditioned media was determined by ELISA for HBD2 (Peprotech, Rocky Hill, NJ), HBD3 (Peprotech), and cathelicidin (LL-37; Hycult, Plymouth Meeting, PA) according to manufacturer’s protocols. NHDF transfected with shRNA constructs were plated at 33,000 cells/well in 24 well plates in FGM-2 media. The next day, the media was changed to DMEM + 10% FBS and the cells were stimulated with PALA (25 µM) for 24 hours. Cell supernatants were collected and antibacterial activity was assessed in triplicate by combining 170 µL of conditioned media with 100,000 cfu for 1 h in a total volume of 180 µL. Bacterial viability was determined through serial dilution and the plating of duplicate samples on LB agar plates.
Skin was excised from the back or upper buttocks of Yorkshire pigs according to relevant regulatory guidelines and regulations in a protocol approved by the Cleveland Clinic Institutional Animal Care and Use Committee (IACUC#2014-1341). De-identified residual/redundant human skin tissue was collected from individuals undergoing elective breast reduction, breast reconstruction surgery, thighplasty, facelift surgery or abdominoplasty at the Cleveland Clinic under a protocol approved by the Cleveland Clinic Institutional Review Board (IRB#13-1381) in accordance with the relevant regulatory guidelines and regulations. Underlying fat and fascia were removed by scalpel and then the skin was rinsed twice in PBS. Skin samples were washed in DMEM + 2 × penicillin/streptomycin/Amphotericin B for 1 h at 37 °C. The samples were placed in DMEM + 10% FBS and allowed to rest overnight at 37 °C. The following day, biopsies (6 mm) were cut, the epidermal layer perforated three times either with a sterile 25 g needle (pig) or GREER allergy test needles (human), and placed on Transwell inserts (6 µM pore size) in 24 well plates with DMEM + 10% FBS in the lower chamber or gauze sponge in 6 well plates with DMEM + 10% FBS. The apical surface was infected with SAP227, P. aeruginosa, or A. baumannii (3 million cfu/explant). After 1 h, Aquaphor, 2%(w/w) PALA in Aquaphor (Cleveland Clinic Investigational Drug Service), or Neosporin was applied to the apical surface in triplicate and incubated for an additional 4 hours or 24 hours. Tissue was homogenized in 2 mL PBS using an Omni-GLH homogenizer (Thomas Scientific, Swedesboro, NJ) and bacterial viability determined in serial dilutions plated in duplicate on LB agar plates. Samples infected with SAP227 and treated with Aquaphor, 2% PALA, or Neosporin were embedded for immunohistochemistry and homogenized for ELISA assays. AMP levels in tissue homogenates was determined by ELISA for HBD2 (Peprotech, Rocky Hill, NJ), HBD3 (Peprotech), and cathelicidin (LL-37; Hycult, Plymouth Meeting, PA) according to manufacturer’s protocols.
Infected human skin explants treated with Aquaphor or 2% PALA were fixed in Histochoice. Next, paraffin embedded samples were sectioned and stained for HBD2, HBD3, or LL-37. Briefly, dewaxed and rehydrated sections were first subjected to antigen retrieval in sodium citrate buffer using a steamer for 25 minutes. Primary antibody staining was performed at 4 °C overnight in a humidifying chamber. Labelled polymer-HRP anti-rabbit (Dako, K4011), biotinylated secondary goat anti-mouse (EMD Millipore, IHC Select, 20775), and streptavidin-HRP (EMD Millipore, IHC Select, 20774) were used as detection reagents/secondary antibodies. Vina green chromogen (Biocare Medical, BRR807A) was used to visualize protein levels. Aperio AT2 (Leica Biosystems) was used to scan the slides.
All statistical analyses were performed on GraphPad Prism software (Version 5.02). One-way or two-way Analysis of Variance (ANOVA) with post-hoc Bonferroni or Tukey’s multiple comparison test was used to determine significance of datasets with multiple variables. For datasets with two variables, unpaired, two-tailed, Students t-test or Wilcoxon matched-pairs signed rank test was used to determine significance. Details of tests used for specific experiments have been included in the figure legends. Results are representative of a minimum of three independent experiments performed in triplicate.
All data generated or analyzed during this study are included in this published article and its supplementary information files.
Tanwar, J., Das, S., Fatima, Z. & Hameed, S. Multidrug resistance: an emerging crisis. Interdiscip Perspect Infect Dis 2014, 541340, https://doi.org/10.1155/2014/541340 (2014).
CDC. Antibiotic Resistance Threats in the United States, 2013. Centers for Disease Control and Prevention, U.S. Department of Health and Human Services (2013).
Rice, L. B. Federal funding for the study of antimicrobial resistance in nosocomial pathogens: no ESKAPE. J Infect Dis 197, 1079–1081, https://doi.org/10.1086/533452 (2008).
Rice, L. B. Progress and challenges in implementing the research on ESKAPE pathogens. Infect Control Hosp Epidemiol 31(Suppl 1), S7–10, https://doi.org/10.1086/655995 (2010).
Santajit, S. & Indrawattana, N. Mechanisms of Antimicrobial Resistance in ESKAPE Pathogens. Biomed Res Int 2016, 2475067, https://doi.org/10.1155/2016/2475067 (2016).
Jatana, S. & DeLouise, L. A. Understanding engineered nanomaterial skin interactions and the modulatory effects of ultraviolet radiation skin exposure. Wiley Interdiscip Rev Nanomed Nanobiotechnol 6, 61–79, https://doi.org/10.1002/wnan.1244 (2014).
Afshar, M. & Gallo, R. L. Innate immune defense system of the skin. Vet Dermatol 24(32-38), e38–39, https://doi.org/10.1111/j.1365-3164.2012.01082.x (2013).
Nestle, F. O., Di Meglio, P., Qin, J. Z. & Nickoloff, B. J. Skin immune sentinels in health and disease. Nat Rev Immunol 9, 679–691, https://doi.org/10.1038/nri2622 (2009).
Kaplan, D. H. In vivo function of Langerhans cells and dermal dendritic cells. Trends Immunol 31, 446–451, https://doi.org/10.1016/j.it.2010.08.006 (2010).
Heath, W. R. & Carbone, F. R. The skin-resident and migratory immune system in steady state and memory: innate lymphocytes, dendritic cells and T cells. Nat Immunol 14, 978–985, https://doi.org/10.1038/ni.2680 (2013).
O’Neill, L. Toll-like receptors and NOD-like receptors: key drivers of innate immunity and inflammation. Immunology 135, 8–8 (2011).
Strbo, N., Yin, N. & Stojadinovic, O. Innate and Adaptive Immune Responses in Wound Epithelialization. Adv Wound Care (New Rochelle) 3, 492–501, https://doi.org/10.1089/wound.2012.0435 (2014).
Kluwe, J., Mencin, A. & Schwabe, R. F. Toll-like receptors, wound healing, and carcinogenesis. J Mol Med (Berl) 87, 125–138, https://doi.org/10.1007/s00109-008-0426-z (2009).
Finlay, B. B. & Hancock, R. E. Can innate immunity be enhanced to treat microbial infections? Nat Rev Microbiol 2, 497–504, https://doi.org/10.1038/nrmicro908 (2004).
Geddes, K., Magalhaes, J. G. & Girardin, S. E. Unleashing the therapeutic potential of NOD-like receptors. Nat Rev Drug Discov 8, 465–479, https://doi.org/10.1038/nrd2783 (2009).
Richmond, A. L. et al. The nucleotide synthesis enzyme CAD inhibits NOD2 antibacterial function in human intestinal epithelial cells. Gastroenterology 142, 1483–1492 e1486, https://doi.org/10.1053/j.gastro.2012.02.040 (2012).
Alnabhani, Z. et al. Pseudomonas fluorescens alters the intestinal barrier function by modulating IL-1beta expression through hematopoietic NOD2 signaling. Inflamm Bowel Dis 21, 543–555, https://doi.org/10.1097/MIB.0000000000000291 (2015).
Bist, P. et al. The Nod1, Nod2, and Rip2 axis contributes to host immune defense against intracellular Acinetobacter baumannii infection. Infect Immun 82, 1112–1122, https://doi.org/10.1128/IAI.01459-13 (2014).
Hruz, P. et al. NOD2 contributes to cutaneous defense against Staphylococcus aureus through alpha-toxin-dependent innate immune activation. Proc Natl Acad Sci USA 106, 12873–12878, https://doi.org/10.1073/pnas.0904958106 (2009).
Strober, W. & Watanabe, T. NOD2, an intracellular innate immune sensor involved in host defense and Crohn’s disease. Mucosal Immunol 4, 484–495, https://doi.org/10.1038/mi.2011.29 (2011).
Campbell, L., Williams, H., Crompton, R. A., Cruickshank, S. M. & Hardman, M. J. Nod2 deficiency impairs inflammatory and epithelial aspects of the cutaneous wound-healing response. J Pathol 229, 121–131, https://doi.org/10.1002/path.4095 (2013).
Rohrl, J., Yang, D., Oppenheim, J. J. & Hehlgans, T. Identification and Biological Characterization of Mouse beta-defensin 14, the orthologue of human beta-defensin 3. J Biol Chem 283, 5414–5419, https://doi.org/10.1074/jbc.M709103200 (2008).
Voss, E. et al. NOD2/CARD15 mediates induction of the antimicrobial peptide human beta-defensin-2. J Biol Chem 281, 2005–2011, https://doi.org/10.1074/jbc.M511044200 (2006).
Warner, N. et al. A genome-wide siRNA screen reveals positive and negative regulators of the NOD2 and NF-kappaB signaling pathways. Sci Signal 6, rs3, https://doi.org/10.1126/scisignal.2003305 (2013).
Collins, K. D. & Stark, G. R. Aspartate transcarbamylase. Interaction with the transition state analogue N-(phosphonacetyl)-L-aspartate. J Biol Chem 246, 6599–6605 (1971).
Plaut, R. D., Mocca, C. P., Prabhakara, R., Merkel, T. J. & Stibitz, S. Stably luminescent Staphylococcus aureus clinical strains for use in bioluminescent imaging. PLoS One 8, e59232, https://doi.org/10.1371/journal.pone.0059232 (2013).
Deshmukh, H. S. et al. Critical role of NOD2 in regulating the immune response to Staphylococcus aureus. Infect Immun 77, 1376–1382, https://doi.org/10.1128/IAI.00940-08 (2009).
Ratner, A. J., Aguilar, J. L., Shchepetov, M., Lysenko, E. S. & Weiser, J. N. Nod1 mediates cytoplasmic sensing of combinations of extracellular bacteria. Cell Microbiol 9, 1343–1351, https://doi.org/10.1111/j.1462-5822.2006.00878.x (2007).
Munguia, J. & Nizet, V. Pharmacological Targeting of the Host-Pathogen Interaction: Alternatives to Classical Antibiotics to Combat Drug-Resistant Superbugs. Trends Pharmacol Sci 38, 473–488, https://doi.org/10.1016/j.tips.2017.02.003 (2017).
Rios, A. C. et al. Alternatives to overcoming bacterial resistances: State-of-the-art. Microbiol Res 191, 51–80, https://doi.org/10.1016/j.micres.2016.04.008 (2016).
Antimicrobial Resistance: Tackling a Crisis for the Heath and Wealth of Nations., (HM Government, 2014).
Hancock, R. E., Nijnik, A. & Philpott, D. J. Modulating immunity as a therapy for bacterial infections. Nat Rev Microbiol 10, 243–254, https://doi.org/10.1038/nrmicro2745 (2012).
Helbig, E. T., Opitz, B. & Sander, L. E. Adjuvant immunotherapies as a novel approach to bacterial infections. Immunotherapy 5, 365–381, https://doi.org/10.2217/imt.13.17 (2013).
Yu, F. S. et al. Flagellin stimulates protective lung mucosal immunity: role of cathelicidin-related antimicrobial peptide. J Immunol 185, 1142–1149, https://doi.org/10.4049/jimmunol.1000509 (2010).
Williams, H. et al. Cutaneous Nod2 expression regulates the skin microbiome and wound healing in a murine model. J Invest Dermatol, https://doi.org/10.1016/j.jid.2017.05.029 (2017).
Polk, H. C. Jr. et al. Nonspecific enhancement of host defenses against infection: experimental evidence of a new order of efficacy and safety. Surgery 90, 376–380 (1981).
Fidler, I. J., Brown, N. O. & Hart, I. R. Species variability for toxicity of free and liposome-encapsulated muramyl peptides administered intravenously. Journal of biological response modifiers 4, 298–309 (1985).
Darcissac, E. C. et al. The synthetic immunomodulator murabutide controls human immunodeficiency virus type 1 replication at multiple levels in macrophages and dendritic cells. Journal of virology 74, 7794–7802 (2000).
Amiel, C. et al. Clinical tolerance and immunologic effects after single or repeated administrations of the synthetic immunomodulator murabutide in HIV-1-infected patients. Journal of acquired immune deficiency syndromes (1999) 30, 294–305 (2002).
Hua, L. et al. Assessment of an anti-alpha-toxin monoclonal antibody for prevention and treatment of Staphylococcus aureus-induced pneumonia. Antimicrob Agents Chemother 58, 1108–1117, https://doi.org/10.1128/AAC.02190-13 (2014).
Aridis Pharmaceuticals, I. NCT01589185 Safety, Pharmacokinetics and Efficacy of KBSA301 in Severe Pneumonia (S. Aureus). (2016).
Kuo, D. et al. Novel quorum-quenching agents promote methicillin-resistant Staphylococcus aureus (MRSA) wound healing and sensitize MRSA to beta-lactam antibiotics. Antimicrob Agents Chemother 59, 1512–1518, https://doi.org/10.1128/AAC.04767-14 (2015).
Tatara, O., Nakahama, C. & Niki, Y. Synergistic effects of romurtide and cefmenoxime against experimental Klebsiella pneumonia in mice. Antimicrob Agents Chemother 36, 167–171 (1992).
Nizet, V. et al. Innate antimicrobial peptide protects the skin from invasive bacterial infection. Nature 414, 454–457, https://doi.org/10.1038/35106587 (2001).
Cole, A. M. et al. Inhibition of neutrophil elastase prevents cathelicidin activation and impairs clearance of bacteria from wounds. Blood 97, 297–304 (2001).
Nizet, V. Antimicrobial peptide resistance mechanisms of human bacterial pathogens. Curr Issues Mol Biol 8, 11–26 (2006).
Raqib, R. et al. Improved outcome in shigellosis associated with butyrate induction of an endogenous peptide antibiotic. Proc Natl Acad Sci USA 103, 9178–9183, https://doi.org/10.1073/pnas.0602888103 (2006).
Mily, A. et al. Significant Effects of Oral Phenylbutyrate and Vitamin D3 Adjunctive Therapy in Pulmonary Tuberculosis: A Randomized Controlled Trial. PLoS One 10, e0138340, https://doi.org/10.1371/journal.pone.0138340 (2015).
Bergman, P. NCT02178488 Efficacy Study of Vitamin D Supplementation to Meticillin Resistant Staphylococcus Aureus (MRSA) Carriers (D-STAPH). ClinicalTrials.gov (2017).
International Centre for Diarrhoeal Disease Research, B. NCT00800930 Therapeutic Induction of EndogenousAntibiotics. ClinicalTrials.gov (2011).
Haisma, E. M. et al. LL-37-derived peptides eradicate multidrug-resistant Staphylococcus aureus from thermally wounded human skin equivalents. Antimicrob Agents Chemother 58, 4411–4419, https://doi.org/10.1128/AAC.02554-14 (2014).
Mohamed, M. F., Abdelkhalek, A. & Seleem, M. N. Evaluation of short synthetic antimicrobial peptides for treatment of drug-resistant and intracellular Staphylococcus aureus. Sci Rep 6, 29707, https://doi.org/10.1038/srep29707 (2016).
Hata, T. R. & Gallo, R. L. Antimicrobial peptides, skin infections, and atopic dermatitis. Semin Cutan Med Surg 27, 144–150, https://doi.org/10.1016/j.sder.2008.04.002 (2008).
Braff, M. H., Di Nardo, A. & Gallo, R. L. Keratinocytes store the antimicrobial peptide cathelicidin in lamellar bodies. J Invest Dermatol 124, 394–400, https://doi.org/10.1111/j.0022-202X.2004.23443.x (2005).
Yamasaki, K. & Gallo, R. L. Antimicrobial peptides in human skin disease. European Journal of Dermatology 18, 11–21 (2008).
McDonald, C. et al. A role for Erbin in the regulation of Nod2-dependent NF-kappa B signaling. J Biol Chem 280, 40301–40309, https://doi.org/10.1074/jbc.M508538200 (2005).
Ip, W. K. E. et al. Phagocytosis and Phagosome Acidification Are Required for Pathogen Processing and MyD88-Dependent Responses to Staphylococcus aureus. Journal of Immunology 184, 7071–7081, https://doi.org/10.4049/jimmunol.1000110 (2010).
Livak, K. J. & Schmittgen, T. D. Analysis of relative gene expression data using real-time quantitative PCR and the 2(-Delta Delta C(T)) Method. Methods 25, 402–408, https://doi.org/10.1006/meth.2001.1262 (2001).
Homer, C. R., Richmond, A. L., Rebert, N. A., Achkar, J. P. & McDonald, C. ATG16L1 and NOD2 Interact in an Autophagy-Dependent Antibacterial Pathway Implicated in Crohn’s Disease Pathogenesis. Gastroenterology 139, 1630–1641.e2, https://doi.org/10.1053/j.gastro.2010.07.006 (2010).
This work was supported by the Assistant Secretary of Defense for Health Affairs, through the Peer Reviewed Medical Research Program under Award No. W81XWH-16-1-0439 (to C.M.), pilot funding from STERIS Corporation (to C.M.), and philanthropic donations from Guy and Mary Jo McDonald. Opinions, interpretations, conclusions, and recommendations are those of the authors and are not necessarily endorsed by the study sponsors. We thank the National Cancer Institute Developmental Therapeutics Program for providing PALA for our studies. We also thank Drs. Michelle Longworth, Roger Plaut, and Gabriel Nuñez for their gifts of bacterial strains and plasmids. We appreciate the technical support of Dr. Judy Drazba and the Cleveland Clinic Lerner Research Institute Imaging Core, as well as the writing of the macro to analyze our live cell images by Dr. Faris El-Khider. Finally, we thank the members of the McDonald and Papay laboratories for their support.
The authors declare no competing interests.
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Jatana, S., Homer, C.R., Madajka, M. et al. Pyrimidine synthesis inhibition enhances cutaneous defenses against antibiotic resistant bacteria through activation of NOD2 signaling. Sci Rep 8, 8708 (2018). https://doi.org/10.1038/s41598-018-27012-0