Next Article in Journal
Roles for Selenoprotein I and Ethanolamine Phospholipid Synthesis in T Cell Activation
Next Article in Special Issue
Severe Natural Outbreak of Cryptocaryon irritans in Gilthead Seabream Produces Leukocyte Mobilization and Innate Immunity at the Gill Tissue
Previous Article in Journal
Glucocorticoid Receptor Signaling in Diabetes
 
 
Search for Articles:
Title / Keyword
Author / Affiliation / Email
Journal
Article Type
 
 
Advanced Search
 
Section
Special Issue
Volume
Issue
Number
Page
 
Journals
IJMS
Volume 22
Issue 20
10.3390/ijms222011172
ijms-logo
Submit to this Journal Review for this Journal Propose a Special Issue
► Article Menu

Article Menu

share Share announcement Help format_quote Cite question_answer Discuss in SciProfiles thumb_up
...
Endorse textsms
...
Comment
first_page
settings
Order Article Reprints
Font Type:
Arial Georgia Verdana
Font Size:
Aa Aa Aa
Line Spacing:
Column Width:
Background:
Review

Host Defense Peptides: Dual Antimicrobial and Immunomodulatory Action

by
Matthew Drayton
1,2,
Julia P. Deisinger
3,
Kevin C. Ludwig
3,
Nigare Raheem
1,
Anna Müller
3,
Tanja Schneider
3 and
Suzana K. Straus
1,*
1
Department of Chemistry, University of British Columbia, 2036 Main Mall, Vancouver, BC V6T 1Z1, Canada
2
The Centre for Blood Research, University of British Columbia, 2350 Health Sciences Mall, Vancouver, BC V6T 1Z3, Canada
3
Institute for Pharmaceutical Microbiology, University Hospital Bonn, University of Bonn, Meckenheimer Allee 168, 53115 Bonn, Germany
*
Author to whom correspondence should be addressed.
Int. J. Mol. Sci. 2021, 22(20), 11172; https://doi.org/10.3390/ijms222011172
Submission received: 20 September 2021 / Revised: 8 October 2021 / Accepted: 13 October 2021 / Published: 16 October 2021
(This article belongs to the Special Issue Antimicrobial Peptides and Immunology)
Browse Figures
Versions Notes

Abstract

:
The rapid rise of multidrug-resistant (MDR) bacteria has once again caused bacterial infections to become a global health concern. Antimicrobial peptides (AMPs), also known as host defense peptides (HDPs), offer a viable solution to these pathogens due to their diverse mechanisms of actions, which include direct killing as well as immunomodulatory properties (e.g., anti-inflammatory activity). HDPs may hence provide a more robust treatment of bacterial infections. In this review, the advent of and the mechanisms that lead to antibiotic resistance will be described. HDP mechanisms of antibacterial and immunomodulatory action will be presented, with specific examples of how the HDP aurein 2.2 and a few of its derivatives, namely peptide 73 and cG4L73, function. Finally, resistance that may arise from a broader use of HDPs in a clinical setting and methods to improve biocompatibility will be briefly discussed.

Graphical Abstract

1. Antibiotic Resistance

The discovery of antibiotic agents has been deemed one of the most impactful advances in modern medicine. Indeed, the administration of penicillin, first discovered by Sir Alexander Fleming in 1928, began what is known as the “era of antibiotics”, where once-deadly infections caused even by a small cut in the skin could be effectively treated [1,2]. The period of rapid antibiotic discovery that occurred shortly thereafter (termed the 1950s “golden era”) contributed to the pivotal role of these agents in medicine and surgery today.
However, specific resistance of the infectious bacteria to these drugs emerged rapidly. In fact, one of the factors initiating the large-scale discovery of antibiotics in the golden era was the need to combat infections by penicillin-resistant bacteria [3,4], which were identified even before the widespread administration of penicillin in World War II [3]. Importantly, β-lactams—a family of chemically modified penicillin derivatives resistant to cleavage by penicillinases, or beta-lactamases—were developed during this period. To date, resistance has been identified for nearly all developed antibiotics [3,4,5]. Even bacteria resistant to vancomycin, a promising antibiotic used for the treatment of methicillin-resistant Staphylococcus aureus (MRSA) that displayed very little resistance generation in a laboratory setting, were identified only 7 years after the introduction of the drug into clinical practice in 1972 [4].
Once the traditional approach of modifying existing antibiotics began to lose its efficacy against these multidrug-resistant (MDR) organisms, many large pharmaceutical companies began to abandon antibiotic discovery programs in the 1980s for other avenues promising greater profits [6]. Stricter regulatory barriers by, e.g., the United States Food and Drug Administration (FDA) exacerbated the issue, with reductions in the number of approved antibiotics significantly increasing between 1983 and 2007 meaning even effective antibiotics could be rejected for commercial use [4]. As such, the number of novel antibiotics approved by the FDA each year has greatly decreased [4,7,8]. Promisingly, though, the approval of 9 new drugs between 2018 and 2019, a significant increase from previous years, suggests this may improve in the near future [8].
Nevertheless, the slow development and approval of effective antibiotics means bacterial infections are once again posing a serious threat to global human health. Experts in the field have estimated that, if left unchecked, these antibiotic resistant-pathogens could cause infection-related deaths to rise to levels observed during the Victorian era or cost 10 million lives per year by 2050 [5,9], which some suggest might actually be an underestimate [10]. Further, on a topical note, many are concerned that the recent COVID-19 pandemic may exacerbate resistance and increase this number, as antibiotics are being heavily overprescribed to COVID-19 patients even when only a small proportion (estimated to be 6.9% [11]) also display bacterial co-infection [11,12,13]. As such, it is of utmost importance and urgency to develop novel treatments for these infections, as well as more tightly regulate the current excessive use of antibiotics in healthcare and other fields, such as agriculture, that facilitate resistance generation [3,4].

2. Bacterial Cells

A key characteristic of an effective antibiotic is its ability to selectively target bacterial cells. Thus, it is important to understand the makeup of these organisms and how they differ from eukaryotic cells. Bacteria are generally categorized into one of two groups based on the composition of their cell walls. These are termed Gram-positive and Gram-negative bacteria, the namesakes of which derive from the bacteriologist Hans Christian Gram, who developed the staining technique used to differentiate between the two [14]. Gram-negative bacteria, in contrast with Gram-positive, contain an outer membrane that is essential for protecting the cell from the environment (Figure 1a) [15]. This outer membrane contains fewer phospholipids than the inner membrane, which themselves are restricted to the inner leaflet, and instead is made up mainly of glycolipids. Of particular note is the glycolipid lipopolysaccharide (LPS), which promotes the secretion of pro-inflammatory cytokines by immune cells [15]. These cytokines are responsible for coordinating the body’s innate defense against infection; however, when released in sudden, large amounts, they can result in sepsis, leading to tissue and organ damage that may be fatal [15,16].
Below the outer membrane of Gram-negative bacteria is a thin, rigid layer of peptidoglycan, a polymer consisting of alternating amino sugars called N-acetylglucosamine and N-acetylmuramic acid [15]. Together, the outer membrane and peptidoglycan wall stabilize the inner membrane, preventing lysis by counterbalancing the high osmotic pressure found within the cell. The periplasm, a viscous space between the inner and outer membranes, is responsible for housing enzymes involved in cell wall maintenance and for sequestering destructive enzymes, such as RNAse [15].
Conversely, Gram-positive bacteria do not contain an outer membrane (Figure 1b). Instead, a much thicker layer of peptidoglycan surrounds the inner membrane [15]. Unique to Gram-positive bacteria, this layer also contains anionic glycopolymers that account for a large proportion of the wall’s mass and play important roles in, among others, membrane stability, membrane function and intercellular interactions [15,17]. One major group of these polymers is teichoic acids, which can be further categorized into lipoteichoic acids and wall teichoic acids (WTAs) depending on their anchoring to lipids of the inner membrane or to peptidoglycan, respectively [17]. These acids impart a generalized negative charge to the surface of the bacteria, a unique feature that is importantly not displayed by mammalian cells (Figure 1c) [18]. Gram-negative bacteria likewise have an overall negative charge due to the phosphate groups present in LPS [19].

3. Mechanisms of Antibiotic Resistance

The unique physiological characteristics of bacterial cells can be taken advantage of in the development of antibiotics. In particular, there are five major targets conventionally exploited by antibiotics: the bacterial cell membrane, the peptidoglycan cell wall, nucleic acid synthesis, protein synthesis and metabolic pathways [20,21].
However, as previously mentioned, many bacteria have quickly developed methods to resist the action of conventional antibiotics. Resistance can be intrinsic—i.e., arising from the inherent structural features of a bacterial species, such as efflux pumps that can remove drugs from the cytosol, absent targeting structures and differences in cytoplasmic membrane structures (especially between Gram-positive and Gram-negative bacteria, as discussed earlier); or acquired or developed, either through the acquisition of genetic material from other bacterial species (horizontal gene transfer, HGT) or by mutations in their own chromosomal DNA [22,23]. In fact, the discovery of this genetic mechanism of acquired resistance, first posited in the mid-1950s, completely transformed the field of microbiology and resulted in a much better understanding of the generation and treatment of drug-resistant pathogens [3].
In general, three main mechanisms of acquired antibiotic resistance have been identified: 1. reduction of intracellular antibiotic concentration via drug efflux and/or decreased membrane penetration; 2. modification of antibiotic targets, either genetically or by post-translational modification; and 3. inactivation of the antibiotic itself by degradation (e.g., hydrolysis) or by biochemical modification (e.g., acetylation and phosphorylation) [22,23]. These mechanisms are summarized in Figure 2.
Due to the limited availability of small molecule antibiotics and their restricted mechanisms of action and activity spectra, there has been great interest in identifying novel antibiotic alternatives for the treatment of existing and emerging MDR bacteria [24]. In recent years, the development of novel antibiotics has exhibited a shift towards the discovery of novel bacterial targets (e.g., new binding sites in bacterial ribosomes, the cell wall, metabolic pathways, etc.) and towards the development of non-traditional approaches to combat infections (e.g., antivirulent, adjunctive, preventative, microbiota-modulating and immunomodulating strategies) [6,24,25]. Interestingly, a large fraction of the agents currently in preclinical development focus on pathogen-specific treatment, which has not generally been prevalent in antibiotic history [6]. One particular promising family of compounds that has garnered much interest as both direct acting and immunomodulating therapies against infection is host defense peptides (HDPs), discussed below.

4. Host Defense Peptides

Antimicrobial peptides (AMPs), now more commonly referred to as HDPs, have been identified as key compounds in the host defense systems of virtually all organisms across the three domains of life. In addition to displaying activity against a broad spectrum of bacteria and other pathogenic species [26,27], many HDPs also favorably modulate the host’s immune and inflammatory responses to infection [28,29]. Moreover, HDPs have been associated with slower resistance generation compared to conventional antibiotics [30,31] (more on this in Section 4.3) and have also been found to be effective against biofilm-associated bacteria [24,28,32,33]. These properties highlight clear advantages of HDPs over conventional small-molecule antibiotics, but their success in being translated into clinical practice has been low due to a number of inherent biocompatibility shortcomings, as discussed in Section 4.3.

4.1. Structures and Classes

In nature, HDPs are produced both ribosomally and nonribosomally, with the majority of the latter being synthesized by bacterial species [34]. HDPs synthesized by ribosomal translation of mRNA are found more widely, from bacteria to higher order life forms, and have been found to play critical roles in the innate immunity of these organisms. In humans and other mammals, many ribosomal HDPs are stored within immune cells, specifically in the granules of neutrophils, where they can be released locally at sites of infection and inflammation; or they are released in skin and mucosal secretions [34]. Their production is also often tightly regulated, with many being expressed as inactive precursors and later activated by proteolytic cleavage [34]. Expression can be constitutive (e.g., in neutrophils, as discussed), or induced by the presence of pathogen-associated molecular patterns (PAMPs) or cytokines during, e.g., inflammation and infection [34].
Generally speaking, HDPs are short polypeptide sequences ranging from 12–50 amino acids with an overall positive charge (generally ≥ +2) and high hydrophobic character (typically 30–50%) [34,35]. As such, they often possess a large number of tryptophan, lysine and arginine residues. These structural features are responsible for the antimicrobial activity of the compounds: the positive charge enables targeting of bacteria via electrostatic interactions with negatively charged bacterial membranes (see Section 2), while the hydrophobicity facilitates interactions with the phospholipid membrane, which can result in disruption of its integrity or can allow for translocation of the peptide into the cytosol where it can target intracellular processes [34].
A common classification system of HDPs utilizes the peptide’s secondary structure—that is, their propensity to form α-helical, β-sheet or random-coil/extended structures, the first two of which are most common in nature [34,36]. In general, α-helical HDPs are unstructured in solution but form amphiphilic structures when in contact with a biological membrane, whereas β-sheet peptides are more structured in solution due to the presence of disulphide bonds, leading to smaller conformational changes upon interaction with lipid membranes. Even though extended HDPs often possess no secondary structure, they also fold into amphiphilic structures upon membrane interaction and often contain a high number of proline and histidine residues in addition to arginine and tryptophan [34].

4.2. Mechanisms of Action for HDPs

Facilitated by their amphiphilic and cationic structures, many HDPs directly destroy bacteria through initial interactions with the bacterial membrane [34]. This key electrostatic interaction forms between the cationic amino acids in the HDP and the negatively charged components of bacterial membranes, such as anionic phospholipids (phosphatidylglycerol, cardiolipin and phosphatidylserine) found in both Gram-positive and Gram-negative bacterial membranes (Figure 1a,b); and teichoic acids and LPS present in the cell wall and outer membrane of Gram-positive and Gram-negative bacteria, respectively [34]. In contrast, mammalian cell membranes (Figure 1c) possess mainly zwitterionic phospholipids, with negatively charged phospholipids facing the cytoplasm in the inner leaflet of the membrane, if present at all. This difference imparts some selectivity onto the HDP between bacterial and mammalian cells. Interestingly, the loss of this asymmetry in inner and outer leaflets in cancer cells that results in negatively charged phosphatidylserine being found on the outer leaflet is partially responsible for the anticancer activity of some HDPs [36,37]. In addition to electrostatic interactions, certain HDPs, such as nisin and mesenterecin, also interact with the bacterial membrane through receptor-mediated interactions [36,38,39].
The initial interaction with the bacterial membrane is imperative for the direct killing of bacteria by HDPs, which occurs through physical perturbation of the membrane itself and/or through disruption of intracellular processes (e.g., DNA/RNA synthesis, protein synthesis and folding, enzymatic activity, cell wall synthesis, etc.) after translocation through the membrane (Figure 3a) [34]. Once in contact with the membrane, the HDPs form amphiphilic structures (if not present already, as discussed in Section 4.1)—the cationic domains of the peptide interact with the hydrophilic/negatively charged phospholipid head groups, while the hydrophobic domains associate with the hydrophobic fatty acid tails of the lipid bilayer core [34]. Once a sufficient peptide concentration is reached, the HDPs self-assemble at the bacterial membrane, causing membrane permeability either through pore formation (as in the “barrel-stave” and “toroidal pore” models) or through formation of micelles via detergent-like effects (as in the “carpet” model) [34,36]. This membrane permeabilization ultimately leads to leakage of ions and metabolites, which causes depolarization of the transmembrane potential resulting in impaired membrane function (e.g., osmotic regulation) that eventually leads to membrane rupture and lysis [34]. It can also allow for translocation of HDPs into the cytoplasm for intracellular targeting, as previously mentioned. Details pertaining to these mechanisms have been reviewed extensively [32,36,40,41,42,43] and the reader can consult these reviews for further details. Overall, many HDPs likely function through multiple complementary actions, which may be partially responsible for the minimal resistance generated by bacteria toward the compounds [27,34].
In addition to direct bacterial action, many HDPs have been shown to regulate a broad range of immunomodulatory activities that can enhance the host’s response to infection (Figure 3b). These activities include suppression of proinflammatory cytokines and anti-endotoxin activity, which can prevent abnormal and harmful inflammatory conditions (as present in, e.g., sepsis); stimulation of chemotaxis; and immune cell differentiation and activation, which facilitates clearance of bacteria by the host [29,34,36]. Some of these mechanisms will be discussed in detail in the subsections below.

4.2.1. Leukocyte Recruitment

One of the most important mechanisms by which HDPs modulate the immune system is through the enhanced recruitment of leukocytes, i.e., neutrophils, macrophages, mast cells and T cells (Figure 3b(ii,vii)), by the induction of chemokine release [44,45,46,47,48,49,50]. This specific function requires the involvement of several cellular receptors, such as chemokine receptors (e.g., CCR6, CCR2), GPCRs and Toll-like receptors (TLRs) [48]. The HDP LL-37, as well as a number of human β defensins (HBDs) can also function as chemoattractants [29,51,52]; HBD3 specifically has been shown to activate monocytes via TLR1- and TLR2-mediated signaling [53].

4.2.2. Modulation of Neutrophil Function

Alternatively, HDPs can influence the function of neutrophils by stimulating the secretion of neutrophil chemokines, such as interleukin-8 (IL-8) and (growth-regulated oncogene)-α (Gro-α or CXCL1) [54], or the release of neutrophil extracellular traps (NETs) (Figure 3b(iii)). For instance, the HDP LL-37 has been shown to induce the release of neutrophil antimicrobial granule components, including four different human α-defensins, namely human neutrophil peptide 1 (HNP1), HNP2, HNP3 and HNP4 [55]. LL-37 can in addition promote NET formation and consequently help fend off viral infections [56], as well as other pathogens.

4.2.3. Regulation of Inflammation

Some HDPs can act as pro-inflammatory or anti-inflammatory molecules, thereby regulating the inflammation balance and promoting immune homeostasis [40]. They can enhance pro-inflammatory responses to nucleic acids [57] or modulate inflammation through the induction of anti-inflammatory cytokines or the suppression of LPS-induced pro-inflammatory cytokines (Figure 3b(ix,x) [45,58,59]. IDR-1018 has been shown to enhance anti-inflammatory functions while also preserving pro-inflammatory activities needed for the resolution of infection, by driving macrophage differentiation towards an intermediate M1–M2 phenotype [58].

4.2.4. Additional Immunomodulatory Functions

In addition to the functions described above, HDPs have also been implicated in the recruitment of antigen-presenting cells such as monocytes [60], macrophages [61] and dendritic cells [62]. They can also promote phagocytosis [63] and modulate the microbiome [64]. For additional detailed examples, the reader is invited to consult the excellent review by Mookherjee et al. [40] and references therein.

4.2.5. Illustration of the Diversity in HDP Function: From a Natural Peptide to Synthetic Analogues

In order to illustrate how HDP function is related to sequence, we will briefly discuss three related peptides, starting from a natural peptide obtained from amphibians [65].
The aurein peptides are HDPs secreted on the skin of Australian southern bell frogs Litoria aurea and Litoria raniformis [66]. These cationic HDPs form five aurein families, ranging from short and active peptides (Families 1–3) to longer, typically inactive peptides (Families 4 and 5), which can be further categorized into subfamilies based on length and sequence similarity, denoted by an additional number (e.g., aurein 1.2). Families 1–3 have been particularly well studied, displaying broad-spectrum activity with particularly high potency against Gram-positive bacteria [66].
A number of studies [66,67,68,69,70] have shown that aurein 2.2 (Figure 4a), an HDP consisting of 16 amino acids with a net charge of +2 and an amidated C-terminus, functions by forming toroidal pores (Figure 3a(v)) and causing selective leakage of potassium, magnesium and iron. This was initially shown by biophysical studies [67]: (i) circular dichroism (CD) and nuclear magnetic resonance (NMR) were used to show that aurein 2.2 (and its close relative aurein 2.3) forms α-helical structures upon contact with the membrane; (ii) differential scanning calorimetry (DSC) and 31P solid-state NMR were used to show that aurein 2.2 and variants [68,69] perturb the membrane bilayer by forming pores, as also evidenced from oriented CD experiments. Using proteomic profiling and a number of assays to determine ion leakage [70] (including the pyranine-based in vitro ion translocation measurements shown on the right in Figure 4a), the membrane perturbation mechanism of aurein 2.2 was further characterized. The fact that aurein 2.2 functions by creating pores is clearly evident when comparing the ion translocation measurements obtained for this peptide relative to others, such as, e.g., daptomycin, which does not function by forming pores [71] (and hence gives results similar to the control seen in Figure 4a [72]). Overall, killing of bacteria results from the disruption of the transmembrane potential of the bacterial membranes by aurein 2.2. Furthermore, the N-terminus of aurein 2.2 was deemed to be important for function, because truncation of aurein 2.2 by three residues from the C-terminus (aurein 2.2-Δ3) was shown not to hinder its antimicrobial activity [70,73].
Starting from aurein 2.2-Δ3, a number of more active peptides were derived from a library, in which the basic and hydrophobic residues of the original peptide were substituted with arginine and tryptophan, respectively [74]. These amino acids were chosen as they have been shown to facilitate electrostatic interactions between the HDP and the bacterial membrane (in the case of arginine) and to mediate peptide-lipid interactions (in the case of tryptophan) [75,76]. Furthermore, both amino acids have been shown to improve peptide-membrane interactions by the formation of cation-π interactions [76,77]. Two peptides, designated peptide 73 (Figure 4b) and 77, displayed improved bactericidal activity against S. aureus, even though they possessed less α-helicity than aurein 2.2 in model membranes and caused less membrane perturbation as determined by membrane depolarization and ion leakage [66]. Treatment with the peptides resulted in accumulation of UDP-N-acetylmuramic acid (MurNAc) pentapeptide in the cytoplasm indicating that membrane-bound peptidoglycan biosynthesis steps (i.e., lipid II biosynthesis, transglycosylation/transpeptidation or recycling of the bactoprenyl carrier lipid) are inhibited by 73 and 77 (Figure 4b). Likewise, both peptides induced expression of the liaI-lux bioreporter, which is regulated by the cell envelope stress-sensing two-component system LiaRS in Bacillus subtilis [78], confirming the previous findings. Additional experiments are required to narrow down the specific reaction affected and to identify the molecular target of 73 and 77. Altogether, the results suggested that peptides 73 and 77 likely function by permeabilizing through the cell membrane and interacting with other targets, such as those involved in cell wall biosynthesis (Figure 3a(iii)), as other arginine- and tryptophan-rich peptides do [79,80,81,82,83].
The sequence of peptide 73 was further modified, leading to the development of peptides such as cL73 and cG4L73 (Figure 4c). These derivatives contain a cysteine residue at position 1, followed by a linker sequence that can be cleaved by matrix metalloproteinases (MMPs). In the case of cG4L73, four glycine residues are positioned between the cysteine and the linker sequence. These peptides were designed to be conjugated to biocompatible polymers such as polyethylene glycol (PEG) or hyperbranched polyglycerol (HPG) (see Section 4.3). Interestingly, cG4L73 and its PEG conjugate both show immunomodulatory activity as probed by the reduction of LPS-induced pro-inflammatory cytokine TNF-α by macrophage-like cells derived from a human monocytic cell line (Figure 4c, right). This was determined by measuring TNF-α release after 24 h cell co-treatment with LPS alongside peptide or conjugate. Further investigations on how cG4L73 and its PEG conjugate might modulate pro- and anti-inflammatory cytokines (i.e., whether these compounds simply bind to cytokines or directly modulate macrophage M1 and M2 phenotype differentiation [58]) are underway.
Overall, HDPs are thought to provide a more robust treatment of infection through combined antibacterial activity and immune system modulation. This multimodal function of HDPs makes them interesting compounds for the treatment of MDR bacterial infections.

4.3. Shortcomings of HDPs and Mitigation Strategies

Even though HDPs show tremendous promise, their use in the clinic to date is limited [84,85]. Firstly, HDPs are inherently susceptible to protease degradation due to the l-amino acids that make up their structure, severely limiting their bioavailability and circulation time when administered to the body (due to, in particular, the presence of blood and stomach proteases) [86]. Furthermore, their small size results in quick removal from the body by kidney filtration and the reticuloendothelial system [34]. Secondly, many HDPs display cytotoxicity towards host cells, which can result in systemic toxicity [87]. This is thought to be largely due to the hydrophobic faces of the peptides (as indicated by the mean hydrophobic moment, <μH>, Figure 4), a common characteristic often required for antimicrobial activity, which can enable insertion into mammalian cell membranes. Fourthly, because of their charged nature, HDP activity can be compromised by the presence of salt at physiological concentrations [88]. Finally, although HDPs are touted as giving rise to little bacterial resistance [36,89] (most likely due to their relatively limited use in the clinic), examples of resistance mechanisms have been reported [30,40,90,91]. Specifically, bacteria can evade HDPs in manners that are analogous to those illustrated in Figure 2 for antibiotics—in other words, resistance arises in broad terms by (i) degradation of the HDPs, (ii) sequestration, in particular in biofilms, (iii) physico-chemical modifications of the molecules encountered on the path of HDP entry into the bacterial cell, or (iv) efflux pumps (Table 1). However, studies [30,92] suggest that the listed modifications only confer moderate levels of resistance and are relatively non-specific.
Toxicity and low efficacy of HDPs result in non-superiority over conventional antibiotics and have been reported repeatedly as reasons for failure in Phase III clinical trials [24]. Indeed, the majority of peptides being tested clinically are for topical application, where concerns regarding degradation and widespread toxicity are lessened [24,31]. To minimize these disadvantages, HDP sequences have been studied in the presence of, e.g., red blood cells to take into account physiological salt conditions [88,93]. In addition, small molecule HDP mimetics have been investigated [94,95]. Finally, a variety of chemical modifications and delivery vehicles have been harnessed. These are reviewed extensively in a number of excellent publications [96,97] and will only be mentioned briefly here.
In terms of chemical modifications, isomerization [36,98,99]—that is, replacing one or more of the l-amino acids with d-amino acids, cyclization [100,101,102,103,104], lipidation [105,106] or using peptidomimetic approaches [107,108,109,110,111,112] are common strategies. These alterations often offer a benefit to the HDP by reducing protease degradation. A number of drug delivery vehicles showing potential for HDP formulation include lipid encapsulations [113,114], metal nanoparticles [115,116,117,118], synthetic polymers [74,119,120,121,122,123] and natural biomolecules, such as polysaccharides [124,125,126,127,128], polypeptides [129,130], antibodies [131] and DNA nanostructures [132,133]. These encapsulation or conjugation approaches mainly serve to alleviate toxicity issues.
The improvements in biocompatibility, along with the multimodal functions of HDPs [32,36,40], i.e., their ability to follow multiple paths illustrated in Figure 3 in parallel, and the large number of peptide sequences available [32], will ensure that resistance remains moderate and non-specific. This will in turn ensure that HDPs remain effective antimicrobial and immunomodulatory agents for longer periods of time.

5. Conclusions

If left unchecked, the continued rise in multidrug-resistant bacteria will cause infection-related deaths to rise to levels not experienced in generations, where even small injuries might once again be fatal. HDPs, a diverse family of antimicrobial agents produced by virtually all domains of life, present a promising solution to these pathogens due to their high antibacterial activity and, in some cases, auxiliary immunomodulatory properties that potentially provide a more robust response to infection. Indeed, examples were given here of how related peptides, namely the natural aurein 2.2 and its synthetic derivatives peptide 73 and cG4L73, can display a multitude of functions. Additionally, many new approaches are being developed to improve the biocompatibility of HDPs, such as chemical modifications or delivery vehicles. Using a combination of these techniques to improve the limitations of HDPs and considering the vast number of peptide sequences available, it is foreseeable that HDPs will become efficacious therapeutics for the future treatment of multidrug-resistant pathogens, as evidenced by a continued growth in the number of reported clinical studies [2,40,134] (for an up-to-date listing of clinical trials, the website https://clinicaltrials.gov/ct2/home can be consulted).

Author Contributions

M.D. wrote most of the manuscript, made and conducted all experiments on L73 and cG4L73 and their respective PEG conjugates; N.R. synthesized peptide 73 and 77; J.P.D., K.C.L., A.M. and T.S. conducted the peptidoglycan synthesis mechanism of action studies on peptide 73 and 77; S.K.S. oversaw all experiments and contributed to the writing of the manuscript. All authors edited the manuscript. All authors have read and agreed to the published version of the manuscript.

Funding

S.K.S. acknowledges funding from the Natural Sciences and Engineering Research Council of Canada (NSERC). Funding to A.M. and T.S. was provided by the Deutsche Forschungsgemeinschaft (DFG, German Research Foundation)—Project-ID 398967434—TRR 261.

Data Availability Statement

Data supporting previously unreported results can obtained from the corresponding author upon request.

Acknowledgments

The authors would like to acknowledge that some of the figures were created with Biorender.com.

Conflicts of Interest

The authors declare no conflict of interest.

References

  1. Aminov, R.I. A brief history of the antibiotic era: Lessons learned and challenges for the future. Front. Microbiol. 2010, 1, 1–7. [Google Scholar] [CrossRef] [Green Version]
  2. Ting, D.S.J.; Beuerman, R.W.; Dua, H.S.; Lakshminarayanan, R.; Mohammed, I. Strategies in Translating the Therapeutic Potentials of Host Defense Peptides. Front. Immunol. 2020, 11, 983. [Google Scholar] [CrossRef]
  3. Davies, J. Origins and evolution of antibiotic resistance. Microbiologia 1996, 12, 9–16. [Google Scholar] [CrossRef] [Green Version]
  4. Ventola, C.L. The antibiotic resistance crisis: Causes and threats. P T J. 2015, 40, 277–283. [Google Scholar]
  5. Shallcross, L.J.; Howard, S.J.; Fowler, T.; Davies, S.C. Tackling the threat of antimicrobial resistance: From policy to sustainable action. Philos. Trans. R. Soc. B Biol. Sci. 2015, 370, 20140082. [Google Scholar] [CrossRef] [PubMed]
  6. Theuretzbacher, U.; Outterson, K.; Engel, A.; Karlén, A. The global preclinical antibacterial pipeline. Nat. Rev. Microbiol. 2019, 18, 275–2853. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  7. Andrei, S.; Valeanu, L.; Chirvasuta, R.; Stefan, M.-G. New FDA approved antibacterial drugs: 2015–2017. Discoveries 2018, 6, e81. [Google Scholar] [CrossRef] [PubMed]
  8. Andrei, S.; Droc, G.; Stefan, G. FDA approved antibacterial drugs: 2018–2019. Discoveries 2019, 7, e102. [Google Scholar] [CrossRef]
  9. WHO. Antimicrobial resistance. Bull. World Health Organ. 2014, 61, 383–394. [Google Scholar]
  10. Matsunaga, N.; Hayakawa, K. Estimating the impact of antimicrobial resistance. Lancet Glob. Health 2018, 6, e934–e935. [Google Scholar] [CrossRef] [Green Version]
  11. Langford, B.J.; So, M.; Raybardhan, S.; Leung, V.; Westwood, D.; MacFadden, D.R.; Soucy, J.-P.R.; Daneman, N. Bacterial co-infection and secondary infection in patients with COVID-19: A living rapid review and meta-analysis. Clin. Microbiol. Infect. 2020, 26, 1622–1629. [Google Scholar] [CrossRef]
  12. Strathdee, S.A.; Davies, S.C.; Marcelin, J.R. Confronting antimicrobial resistance beyond the COVID-19 pandemic and the 2020 US election. Lancet 2020, 396, 1050–1053. [Google Scholar] [CrossRef]
  13. Hsu, J. How covid-19 is accelerating the threat of antimicrobial resistance. BMJ 2020, 369, 1–2. [Google Scholar]
  14. Coico, R. Gram staining. Curr. Protoc. Microbiol. 2005, 3, A.3C.1–A.3C.2. [Google Scholar] [CrossRef]
  15. Silhavy, T.J.; Kahne, D.; Walker, S. The Bacterial Cell Envelope. Cold Spring Harb. Perspect. Biol. 2010, 2, a000414. [Google Scholar] [CrossRef]
  16. Opal, S.M. Endotoxins and Other Sepsis Triggers. Endotoxemia Endotoxin Shock: Dis. Diagn. Ther. 2010, 167, 14–24. [Google Scholar] [CrossRef]
  17. Swoboda, J.G.; Campbell, J.; Meredith, T.C.; Walker, S. Wall teichoic acid function, biosynthesis, and inhibition. ChemBioChem 2010, 11, 35–45. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  18. Sani, M.A.; Henriques, S.T.; Weber, D.; Separovic, F. Bacteria may cope differently from similar membrane damage caused by the Australian tree frog antimicrobial peptide maculatin 1.1. J. Biol. Chem. 2015, 290, 19853–19862. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  19. Rosenfeld, Y.; Shai, Y. Lipopolysaccharide (Endotoxin)-host defense antibacterial peptides interactions: Role in bacterial resistance and prevention of sepsis. Biochim. Biophys. Acta Biomembr. 2006, 1758, 1513–1522. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  20. Kohanski, M.A.; Dwyer, D.J.; Collins, J.J. How antibiotics kill bacteria: From targets to networks. Nat. Rev. Microbiol. 2010, 8, 423–435. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  21. Hooper, D.C. Mechanisms of action of antimicrobials: Focus on fluoroquinolones. Clin. Infect. Dis. 2001, 32, 9–15. [Google Scholar] [CrossRef]
  22. Blair, J.M.A.; Webber, M.A.; Baylay, A.J.; Ogbolu, D.O.; Piddock, L.J.V. Molecular mechanisms of antibiotic resistance. Nat. Rev. Microbiol. 2015, 13, 42–51. [Google Scholar] [CrossRef]
  23. Reygaert, C.W. An overview of the antimicrobial resistance mechanisms of bacteria. AIMS Microbiol. 2018, 4, 482–501. [Google Scholar] [CrossRef] [PubMed]
  24. Czaplewski, L.; Bax, R.; Clokie, M.; Dawson, M.; Fairhead, H.; Fischetti, V.A.; Foster, S.; Gilmore, B.F.; Hancock, R.; Harper, D.; et al. Alternatives to antibiotics—a pipeline portfolio review. Lancet Infect. Dis. 2016, 16, 239–251. [Google Scholar] [CrossRef] [Green Version]
  25. Theuretzbacher, U.; Piddock, L.J.V. Non-traditional Antibacterial Therapeutic Options and Challenges. Cell Host Microbe 2019, 26, 61–72. [Google Scholar] [CrossRef]
  26. Hancock, R.E.W.; Falla, T.J. Antimicrobial peptides: Broad-spectrum antibiotics from nature. Clin. Microbiol. Infect. 1996, 1, 226–229. [Google Scholar] [CrossRef] [Green Version]
  27. Hancock, R.E.W.; Sahl, H.-G. Antimicrobial and host-defense peptides as new anti-infective therapeutic strategies. Nat. Biotechnol. 2006, 24, 1551–1557. [Google Scholar] [CrossRef]
  28. Magana, M.; Pushpanathan, M.; Santos, A.L.; Leanse, L.; Fernandez, M.; Ioannidis, A.; Giulianotti, M.A.; Apidianakis, Y.; Bradfute, S.; Ferguson, A.L.; et al. The value of antimicrobial peptides in the age of resistance. Lancet Infect. Dis. 2020, 20, e216–e230. [Google Scholar] [CrossRef]
  29. Alford, M.A.; Baquir, B.; Santana, F.L.; Haney, E.F.; Hancock, R.E.W. Cathelicidin Host Defense Peptides and Inflammatory Signaling: Striking a Balance. Front. Microbiol. 2020, 11, 1–18. [Google Scholar] [CrossRef]
  30. Joo, H.S.; Fu, C.I.; Otto, M. Bacterial strategies of resistance to antimicrobial peptides. Philos. Trans. R. Soc. B Biol. Sci. 2016, 371, 20150292. [Google Scholar] [CrossRef] [Green Version]
  31. Koo, H.B.; Seo, J. Antimicrobial peptides under clinical investigation. Pept. Sci. 2019, 111, e24122. [Google Scholar] [CrossRef]
  32. Haney, E.F.; Straus, S.K.; Hancock, R.E.W. Reassessing the Host Defense Peptide Landscape. Front. Chem. 2019, 7, 43. [Google Scholar] [CrossRef] [Green Version]
  33. de la Fuente-Núñez, C.; Reffuveille, F.; Haney, E.F.; Straus, S.K.; Hancock, R.E.W. Broad-Spectrum Anti-biofilm Peptide that Targets a Cellular Stress Response. PLoS Pathog. 2014, 10, e1004152. [Google Scholar] [CrossRef] [Green Version]
  34. Mahlapuu, M.; Håkansson, J.; Ringstad, L.; Björn, C. Antimicrobial peptides: An emerging category of therapeutic agents. Front. Cell. Infect. Microbiol. 2016, 6, 194. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  35. Giuliani, A.; Pirri, G.; Nicoletto, S.F. Antimicrobial peptides: An overview of a promising class of therapeutics. Cent. Eur. J. Biol. 2007, 2, 1–33. [Google Scholar] [CrossRef]
  36. Kumar, P.; Kizhakkedathu, J.N.; Straus, S.K. Antimicrobial peptides: Diversity, mechanism of action and strategies to improve the activity and biocompatibility in vivo. Biomolecules 2018, 8, 4. [Google Scholar] [CrossRef] [Green Version]
  37. Felício, M.R.; Silva, O.N.; Gonçalves, S.; Santos, N.C.; Franco, O.L. Peptides with Dual Antimicrobial and Anticancer Activities. Front. Chem. 2017, 5, 5. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  38. Fleury, Y.; Dayem, M.A.; Montagne, J.J.; Chaboisseau, E.; Le Caer, J.P.; Nicolas, P.; Delfour, A. Covalent structure, synthesis, and structure-function studies of mesentericin Y 10537, a defensive peptide from gram-positive bacteria leuconostoc mesenteroides. J. Biol. Chem. 1996, 271, 14421–14429. [Google Scholar] [CrossRef] [Green Version]
  39. Breukink, E.; De Kruijff, B. The lantibiotic nisin, a special case or not? Biochim. Biophys. Acta Biomembr. 1999, 1462, 223–234. [Google Scholar] [CrossRef] [Green Version]
  40. Mookherjee, N.; Anderson, M.A.; Haagsman, H.P.; Davidson, D.J. Antimicrobial host defence peptides: Functions and clinical potential. Nat. Rev. Drug Discov. 2020, 19, 311–332. [Google Scholar] [CrossRef]
  41. Nguyen, L.T.; Haney, E.F.; Vogel, H.J. The expanding scope of antimicrobial peptide structures and their modes of action. Trends Biotechnol. 2011, 29, 464–472. [Google Scholar] [CrossRef]
  42. Fillion, M.; Valois-Paillard, G.; Lorin, A.; Noël, M.; Voyer, N.; Auger, M. Membrane Interactions of Synthetic Peptides with Antimicrobial Potential: Effect of Electrostatic Interactions and Amphiphilicity. Probiotics Antimicrob. Proteins 2014, 7, 66–74. [Google Scholar] [CrossRef]
  43. Yeaman, M.R.; Yount, N.Y. Mechanisms of antimicrobial peptide action and resistance. Pharmacol. Rev. 2003, 55, 27–55. [Google Scholar] [CrossRef] [Green Version]
  44. Scott, M.G.; Dullaghan, E.; Mookherjee, N.; Glavas, N.; Waldbrook, M.; Thompson, A.; Wang, A.; Lee, K.; Doria, S.; Hamill, P.; et al. An anti-infective peptide that selectively modulates the innate immune response. Nat. Biotechnol. 2007, 25, 465–472. [Google Scholar] [CrossRef]
  45. Hancock, R.E.W.; Nijnik, A.; Philpott, D.J. Modulating immunity as a therapy for bacterial infections. Nat. Rev. Microbiol. 2012, 10, 243–254. [Google Scholar] [CrossRef] [PubMed]
  46. Nijnik, A.; Madera, L.; Ma, S.; Waldbrook, M.; Elliott, M.R.; Easton, D.M.; Mayer, M.L.; Mullaly, S.C.; Kindrachuk, J.; Jenssen, H.; et al. Synthetic Cationic Peptide IDR-1002 Provides Protection against Bacterial Infections through Chemokine Induction and Enhanced Leukocyte Recruitment. J. Immunol. 2010, 184, 2539–2550. [Google Scholar] [CrossRef] [Green Version]
  47. Holly, M.K.; Diaz, K.; Smith, J.G. Defensins in Viral Infection and Pathogenesis. Annu. Rev. Virol. 2017, 4, 369–391. [Google Scholar] [CrossRef] [PubMed]
  48. Hancock, R.E.W.; Haney, E.F.; Gill, E.E. The immunology of host defence peptides: Beyond antimicrobial activity. Nat. Publ. Gr. 2016, 16, 321–334. [Google Scholar] [CrossRef] [PubMed]
  49. Pundir, P.; Catalli, A.; Leggiadro, C.; Douglas, S.E.; Kulka, M. Pleurocidin, a novel antimicrobial peptide, induces human mast cell activation through the FPRL1 receptor. Mucosal Immunol. 2014, 7, 177–187. [Google Scholar] [CrossRef]
  50. Di Nardo, A.; Yamasaki, K.; Dorschner, R.A.; Lai, Y.; Gallo, R.L. Mast Cell Cathelicidin Antimicrobial Peptide Prevents Invasive Group A Streptococcus Infection of the Skin. J. Immunol. 2008, 180, 7565–7573. [Google Scholar] [CrossRef] [Green Version]
  51. Hazlett, L.; Wu, M. Defensins in innate immunity. Cell Tissue Res. 2011, 343, 175–188. [Google Scholar] [CrossRef]
  52. Semple, F.; Dorin, J.R. β-Defensins: Multifunctional modulators of infection, inflammation and more? J. Innate Immun. 2012, 4, 337–348. [Google Scholar] [CrossRef] [PubMed]
  53. Funderburg, N.; Lederman, M.M.; Feng, Z.; Drage, M.G.; Jadlowsky, J.; Harding, C.V.; Weinberg, A.; Sieg, S.F. Human β-defensin-3 activates professional antigen-presenting cells via Toll-like receptors 1 and 2. Proc. Natl. Acad. Sci. USA 2007, 104, 18631–18635. [Google Scholar] [CrossRef] [Green Version]
  54. Hemshekhar, M.; Anaparti, V.; Mookherjee, N. Functions of cationic host defense peptides in immunity. Pharmaceuticals 2016, 9, 40. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  55. Zheng, Y.; Niyonsaba, F.; Ushio, H.; Nagaoka, I.; Ikeda, S.; Okumura, K.; Ogawa, H. Cathelicidin LL-37 induces the generation of reactive oxygen species and release of human α-defensins from neutrophils. Br. J. Dermatol. 2007, 157, 1124–1131. [Google Scholar] [CrossRef] [PubMed]
  56. Tripathi, S.; Wang, G.; White, M.; Rynkiewicz, M.; Seaton, B.; Hartshorn, K. Identifying the critical domain of LL-37 involved in mediating neutrophil activation in the presence of influenza virus: Functional and structural analysis. PLoS ONE 2015, 10, e0133454. [Google Scholar] [CrossRef]
  57. Lande, R.; Pietraforte, I.; Mennella, A.; Palazzo, R.; Spinelli, F.; Giannakakis, K.; Spadaro, F.; Falchi, M.; Riccieri, V.; Stefanantoni, K.; et al. Complementary effects of carbamylated and citrullinated ll37 in autoimmunity and inflammation in systemic lupus erythematosus. Int. J. Mol. Sci. 2021, 22, 1650. [Google Scholar] [CrossRef]
  58. Pena, O.M.; Afacan, N.; Pistolic, J.; Chen, C.; Madera, L.; Falsafi, R.; Fjell, C.; Hancock, R. Synthetic Cationic Peptide IDR-1018 Modulates Human Macrophage Differentiation. PLoS ONE 2013, 8, e52449. [Google Scholar] [CrossRef] [Green Version]
  59. Bevins, C.L.; Salzman, N.H. Paneth cells, antimicrobial peptides and maintenance of intestinal homeostasis. Nat. Rev. Microbiol. 2011, 9, 356–368. [Google Scholar] [CrossRef]
  60. Cai, J.; Cui, X.; Wang, X.; You, L.; Ji, C.; Cao, Y. A Novel Anti-Infective Peptide BCCY-1 With Immunomodulatory Activities. Front. Immunol. 2021, 12, 713960. [Google Scholar] [CrossRef]
  61. He, X.; Yang, Y.; Mu, L.; Zhou, Y.; Chen, Y.; Wu, J.; Wang, Y.; Yang, H.; Li, M.; Xu, W.; et al. A frog-derived immunomodulatory peptide promotes cutaneous wound healing by regulating cellular response. Front. Immunol. 2019, 10, 2421. [Google Scholar] [CrossRef] [Green Version]
  62. Tian, Y.; Hu, Q.; Zhang, R.; Zhou, B.; Xie, D.; Wang, Y.; Zhang, X.; Yang, L. Rational design of innate defense regulator peptides as tumor vaccine adjuvants. NPJ Vaccines 2021, 6, 1–13. [Google Scholar] [CrossRef]
  63. Peng, L.; Scheenstra, M.R.; van Harten, R.M.; Haagsman, H.P.; Veldhuizen, E.J.A. The immunomodulatory effect of cathelicidin-B1 on chicken macrophages. Vet. Res. 2020, 51, 122. [Google Scholar] [CrossRef]
  64. Xiang, X.-W.; Zheng, H.-Z.; Wang, R.; Chen, H.; Xiao, J.-X.; Zheng, B.; Liu, S.-L.; Ding, Y.-T. Ameliorative Effects of Peptides Derived from Oyster (Crassostrea gigas) on Immunomodulatory Function and Gut Microbiota Structure in Cyclophosphamide-Treated Mice. Mar. Drugs 2021, 19, 456. [Google Scholar] [CrossRef]
  65. Bhattacharjya, S.; Straus, S.K. Design, engineering and discovery of novel α-helical and β-boomerang antimicrobial peptides against drug resistant bacteria. Int. J. Mol. Sci. 2020, 21, 5773. [Google Scholar] [CrossRef] [PubMed]
  66. Raheem, N.; Kumar, P.; Lee, E.; Cheng, J.T.; Hancock, R.; Straus, S.K. Insights into the mechanism of action of two analogues of aurein 2.2. Biochim. Biophys. Acta Biomembr. 2020, 1862, 183262. [Google Scholar] [CrossRef] [PubMed]
  67. Pan, Y.-L.; Cheng, J.T.-J.; Hale, J.; Pan, J.; Hancock, R.; Straus, S.K. Characterization of the Structure and Membrane Interaction of the Antimicrobial Peptides Aurein 2.2 and 2.3 from Australian Southern Bell Frogs. Biophys. J. 2007, 92, 2854–2864. [Google Scholar] [CrossRef] [Green Version]
  68. Cheng, J.T.J.; Hale, J.D.; Elliot, M.; Hancock, R.E.W.; Straus, S.K. Effect of membrane composition on antimicrobial peptides aurein 2.2 and 2.3 from australian southern bell frogs. Biophys. J. 2009, 96, 552–565. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  69. Cheng, J.T.J.; Hale, J.D.; Elliott, M.; Hancock, R.E.W.; Straus, S.K. The importance of bacterial membrane composition in the structure and function of aurein 2.2 and selected variants. Biochim. Biophys. Acta Biomembr. 2011, 1808, 622–633. [Google Scholar] [CrossRef] [Green Version]
  70. Wenzel, M.; Senges, C.H.R.; Zhang, J.; Suleman, S.; Nguyen, M.; Kumar, P.; Chiriac, A.I.; Stepanek, J.J.; Raatschen, N.; May, C.; et al. Antimicrobial Peptides from the Aurein Family Form Ion-Selective Pores inBacillus subtilis. ChemBioChem 2015, 16, 1101–1108. [Google Scholar] [CrossRef] [PubMed]
  71. Grein, F.; Müller, A.; Scherer, K.M.; Liu, X.; Ludwig, K.C.; Klöckner, A.; Strach, M.; Sahl, H.-G.; Kubitscheck, U.; Schneider, T. Ca2+-Daptomycin targets cell wall biosynthesis by forming a tripartite complex with undecaprenyl-coupled intermediates and membrane lipids. Nat. Commun. 2020, 11, 1–11. [Google Scholar] [CrossRef] [Green Version]
  72. Zhang, J.; Scoten, K.; Straus, S.K. Daptomycin Leakage Is Selective. ACS Infect. Dis. 2016, 2, 682–687. [Google Scholar] [CrossRef] [PubMed]
  73. Cheng, J.T.; Hale, J.D.; Kindrachuk, J.; Jessen, H.; Elliott, M.; Hancock, R.E.; Straus, S.K. Importance of Residue 13 and the C-Terminus for the Structure and Activity of the Antimicrobial Peptide Aurein 2.2. Biophys. J. 2010, 99, 2926–2935. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  74. Kumar, P.; Takayesu, A.; Abbasi, U.; Kalathottukaren, M.T.; Abbina, S.; Kizhakkedathu, J.N.; Straus, S.K. Antimicrobial Peptide-Polymer Conjugates with High Activity: Influence of Polymer Molecular Weight and Peptide Sequence on Antimicrobial Activity, Proteolysis, and Biocompatibility. ACS Appl. Mater. Interfaces 2017, 9, 37575–37586. [Google Scholar] [CrossRef] [PubMed]
  75. Haney, E.F.; Nguyen, L.T.; Schibli, D.J.; Vogel, H.J. Design of a novel tryptophan-rich membrane-active antimicrobial peptide from the membrane-proximal region of the HIV glycoprotein, gp41. Beilstein J. Org. Chem. 2012, 8, 1172–1184. [Google Scholar] [CrossRef] [PubMed]
  76. Chan, D.I.; Prenner, E.J.; Vogel, H.J. Tryptophan- and arginine-rich antimicrobial peptides: Structures and mechanisms of action. Biochim. Biophys. Acta Biomembr. 2006, 1758, 1184–1202. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  77. Jing, W.; Demcoe, A.R.; Vogel, H.J. Conformation of a Bactericidal Domain of Puroindoline a: Structure and Mechanism of Action of a 13-Residue Antimicrobial Peptide. J. Bacteriol. 2003, 185, 4938–4947. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  78. Mascher, T.; Zimmer, S.L.; Smith, T.-A.; Helmann, J.D. Antibiotic-Inducible Promoter Regulated by the Cell Envelope Stress-Sensing Two-Component System LiaRS of Bacillus subtilis. Antimicrob. Agents Chemother. 2004, 48, 2888–2896. [Google Scholar] [CrossRef] [Green Version]
  79. Sugawara, M.; Resende, J.M.; Moraes, C.M.; Marquette, A.; Chich, J.; Metz-Boutigue, M.; Bechinger, B. Membrane structure and interactions of human catestatin by multidimensional solution and solid-state NMR spectroscopy. FASEB J. 2010, 24, 1737–1746. [Google Scholar] [CrossRef] [Green Version]
  80. Hsu, C.-H. Structural and DNA-binding studies on the bovine antimicrobial peptide, indolicidin: Evidence for multiple conformations involved in binding to membranes and DNA. Nucleic Acids Res. 2005, 33, 4053–4064. [Google Scholar] [CrossRef] [Green Version]
  81. Marchand, C.; Krajewski, K.; Lee, H.-F.; Antony, S.; Johnson, A.A.; Amin, R.; Roller, P.; Kvaratskhelia, M.; Pommier, Y. Covalent binding of the natural antimicrobial peptide indolicidin to DNA abasic sites. Nucleic Acids Res. 2006, 34, 5157–5165. [Google Scholar] [CrossRef] [PubMed]
  82. Overhage, J.; Campisano, A.; Bains, M.; Torfs, E.C.W.; Rehm, B.H.A.; Hancock, R.E.W. Human host defense peptide LL-37 prevents bacterial biofilm formation. Infect. Immun. 2008, 76, 4176–4182. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  83. Khafagy, E.-S.; Morishita, M.; Ida, N.; Nishio, R.; Isowa, K.; Takayama, K. Structural requirements of penetratin absorption enhancement efficiency for insulin delivery. J. Control. Release 2010, 143, 302–310. [Google Scholar] [CrossRef]
  84. Jenssen, H.; Hamill, P.; Hancock, R.E.W. Peptide Antimicrobial Agents. Clin. Microbiol. Rev. 2006, 19, 491–511. [Google Scholar] [CrossRef] [Green Version]
  85. Kosikowska, P.; Lesner, A. Antimicrobial peptides (AMPs) as drug candidates: A patent review (2003–2015). Expert Opin. Ther. Pat. 2016, 26, 689–702. [Google Scholar] [CrossRef] [PubMed]
  86. Vlieghe, P.; Lisowski, V.; Martinez, J.; Khrestchatisky, M. Synthetic therapeutic peptides: Science and market. Drug Discov. Today 2010, 15, 40–56. [Google Scholar] [CrossRef]
  87. Haney, E.F.; Hancock, R.E.W. Peptide design for antimicrobial and immunomodulatory applications. Biopolymers 2013, 100, 572–583. [Google Scholar] [CrossRef] [PubMed]
  88. Yang, M.; Zhang, C.; Zhang, M.Z.; Zhang, S. Beta-defensin derived cationic antimicrobial peptides with potent killing activity against gram negative and gram positive bacteria. BMC Microbiol. 2018, 18, 54. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  89. Koehbach, J.; Gani, J.; Hilpert, K.; Craik, D.J. Comparison of a short linear antimicrobial peptide with its disulfide-cyclized and cyclotide-grafted variants against clinically relevant pathogens. Microorganisms 2021, 9, 1249. [Google Scholar] [CrossRef] [PubMed]
  90. Perron, G.G.; Zasloff, M.; Bell, G. Experimental evolution of resistance to an antimicrobial peptide. Proc. R. Soc. B Biol. Sci. 2006, 273, 251–256. [Google Scholar] [CrossRef] [Green Version]
  91. Gonzalez-Avila, L.U.; Loyola-Cruz, M.A.; Hernández-Cortez, C.; Bello-López, J.M.; Castro-Escarpulli, G. Colistin resistance in aeromonas spp. Int. J. Mol. Sci. 2021, 22, 5974. [Google Scholar] [CrossRef] [PubMed]
  92. Bechinger, B.; Gorr, S.U. Antimicrobial Peptides: Mechanisms of Action and Resistance. J. Dent. Res. 2017, 96, 254–260. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  93. Starr, C.G.; He, J.; Wimley, W.C. Host Cell Interactions are a Significant Barrier to the Clinical Utility of Peptide Antibiotics. ACS Chem Biol. 2016, 11, 3391–3399. [Google Scholar] [CrossRef] [Green Version]
  94. Amponnawarat, A.; Chompunud Na Ayudhya, C.; Ali, H. Murepavadin, a Small Molecule Host Defense Peptide Mimetic, Activates Mast Cells via MRGPRX2 and MrgprB2. Front. Immunol. 2021, 12, 689410. [Google Scholar] [CrossRef]
  95. Lin, S.; Wade, J.D.; Liu, S. De Novo Design of Flavonoid-Based Mimetics of Cationic Antimicrobial Peptides: Discovery, Development, and Applications. Acc. Chem. Res. 2021, 54, 104–119. [Google Scholar] [CrossRef] [PubMed]
  96. Cui, Z.; Luo, Q.; Bannon, M.S.; Gray, V.P.; Bloom, T.G.; Clore, M.F.; Hughes, M.A.; Crawford, M.A.; Letteri, R.A. Molecular engineering of antimicrobial peptide (AMP)–polymer conjugates. Biomater. Sci. 2021, 9, 5069–5091. [Google Scholar] [CrossRef]
  97. Drayton, M.; Kizhakkedathu, J.N.; Straus, S.K. Towards Robust Delivery of Antimicrobial Peptides to Combat Bacterial Resistance. Molecules 2020, 25, 3048. [Google Scholar] [CrossRef]
  98. Zhao, Y.; Zhang, M.; Qiu, S.; Wang, J.; Peng, J.; Zhao, P.; Zhu, R.; Wang, H.; Li, Y.; Wang, K.; et al. Antimicrobial activity and stability of the d-amino acid substituted derivatives of antimicrobial peptide polybia-MPI. AMB Express 2016, 6, 122. [Google Scholar] [CrossRef] [Green Version]
  99. Jia, F.; Wang, J.; Peng, J.; Zhao, P.; Kong, Z.; Wang, K.; Yan, W.; Wang, R. D-amino acid substitution enhances the stability of antimicrobial peptide polybia-CP. Acta Biochim. Biophys. Sin. 2017, 49, 916–925. [Google Scholar] [CrossRef] [Green Version]
  100. Spokoyny, A.M.; Zou, Y.; Ling, J.J.; Yu, H.; Lin, Y.-S.; Pentelute, B.L. A Perfluoroaryl-Cysteine SNAr Chemistry Approach to Unprotected Peptide Stapling. J. Am. Chem. Soc. 2013, 135, 5946–5949. [Google Scholar] [CrossRef] [Green Version]
  101. Lautrette, G.; Touti, F.; Lee, H.G.; Dai, P.; Pentelute, B.L. Nitrogen Arylation for Macrocyclization of Unprotected Peptides. J. Am. Chem. Soc. 2016, 138, 8340–8343. [Google Scholar] [CrossRef]
  102. Etayash, H.; Pletzer, D.; Kumar, P.; Straus, S.K.; Hancock, R.E.W. Cyclic Derivative of Host-Defense Peptide IDR-1018 Improves Proteolytic Stability, Suppresses Inflammation, and Enhances in Vivo Activity. J. Med. Chem. 2020, 63, 9228–9236. [Google Scholar] [CrossRef]
  103. Mourtada, R.; Herce, H.D.; Yin, D.J.; Moroco, J.A.; Wales, T.E.; Engen, J.R.; Walensky, L.D. Design of stapled antimicrobial peptides that are stable, nontoxic and kill antibiotic-resistant bacteria in mice. Nat. Biotechnol. 2019, 37, 1186–1197. [Google Scholar] [CrossRef]
  104. Migoń, D.; Neubauer, D.; Kamysz, W. Hydrocarbon Stapled Antimicrobial Peptides. Protein J. 2018, 37, 2–12. [Google Scholar] [CrossRef] [Green Version]
  105. Rounds, T.; Straus, S.K. Lipidation of antimicrobial peptides as a design strategy for future alternatives to antibiotics. Int. J. Mol. Sci. 2020, 21, 9692. [Google Scholar] [CrossRef]
  106. Lombardi, L.; Shi, Y.; Falanga, A.; Galdiero, E.; de Alteriis, E.; Franci, G.; Chourpa, I.; Azevedo, H.S.; Galdiero, S. Enhancing the Potency of Antimicrobial Peptides through Molecular Engineering and Self-Assembly. Biomacromolecules 2019, 20, 1362–1374. [Google Scholar] [CrossRef]
  107. Molchanova, N.; Hansen, P.R.; Franzyk, H. Advances in development of antimicrobial peptidomimetics as potential drugs. Molecules 2017, 22, 1430. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  108. Ghosh, C.; Sarkar, P.; Issa, R.; Haldar, J. Alternatives to Conventional Antibiotics in the Era of Antimicrobial Resistance. Trends Microbiol. 2019, 27, 323–338. [Google Scholar] [CrossRef] [PubMed]
  109. Kowalski, R.P.; Romanowski, E.G.; Yates, K.A.; Mah, F.S. An independent evaluation of a novel peptide mimetic, Brilacidin (PMX30063), for ocular anti-infective. J. Ocul. Pharmacol. Ther. 2016, 32, 23–27. [Google Scholar] [CrossRef] [PubMed]
  110. Kuppusamy, R.; Willcox, M.; Black, D.S.C.; Kumar, N. Short cationic peptidomimetic antimicrobials. Antibiotics 2019, 8, 44. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  111. Luther, A.; Urfer, M.; Zahn, M.; Müller, M.; Wang, S.-Y.; Mondal, M.; Vitale, A.; Hartmann, J.-B.; Sharpe, T.; Monte, F.L.; et al. Chimeric peptidomimetic antibiotics against Gram-negative bacteria. Nature 2019, 576, 452–458. [Google Scholar] [CrossRef] [PubMed]
  112. Molchanova, N.; Nielsen, J.E.; Sørensen, K.B.; Prabhala, B.K.; Hansen, P.R.; Lund, R.; Barron, A.E.; Jenssen, H. Halogenation as a tool to tune antimicrobial activity of peptoids. Sci. Rep. 2020, 10, 1–10. [Google Scholar] [CrossRef] [PubMed]
  113. Martin-Serrano, Á.; Gómez, R.; Ortega, P.; De La Mata, F.J.D. Nanosystems as vehicles for the delivery of antimicrobial peptides (Amps). Pharmaceutics 2019, 11, 448. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  114. Makowski, M.; Silva, Í.C.; Do Amaral, C.P.; Gonçalves, S.; Santos, N.C. Advances in lipid and metal nanoparticles for antimicrobial peptide delivery. Pharmaceutics 2019, 11, 588. [Google Scholar] [CrossRef] [Green Version]
  115. Rajchakit, U.; Sarojini, V. Recent Developments in Antimicrobial-Peptide-Conjugated Gold Nanoparticles. Bioconjug. Chem. 2017, 28, 2673–2686. [Google Scholar] [CrossRef]
  116. Liu, L.; Yang, J.; Xie, J.; Luo, Z.; Jiang, J.; Yang, Y.Y.; Liu, S. The potent antimicrobial properties of cell penetrating peptide-conjugated silver nanoparticles with excellent selectivity for Gram-positive bacteria over erythrocytes. Nanoscale 2013, 5, 3834–3840. [Google Scholar] [CrossRef]
  117. Gao, J.; Na, H.; Zhong, R.; Yuan, M.; Guo, J.; Zhao, L.; Wang, Y.; Wang, L.; Zhang, F. One step synthesis of antimicrobial peptide protected silver nanoparticles: The core-shell mutual enhancement of antibacterial activity. Colloids Surf. B Biointerfaces 2020, 186, 110704. [Google Scholar] [CrossRef]
  118. Lee, B.; Park, J.; Ryu, M.; Kim, S.; Joo, M.; Yeom, J.-H.; Kim, S.; Park, Y.; Lee, K.; Bae, J. Antimicrobial peptide-loaded gold nanoparticle-DNA aptamer conjugates as highly effective antibacterial therapeutics against Vibrio vulnificus. Sci. Rep. 2017, 7, 1–10. [Google Scholar] [CrossRef]
  119. Ekladious, I.; Colson, Y.L.; Grinstaff, M.W. Polymer–drug conjugate therapeutics: Advances, insights and prospects. Nat. Rev. Drug Discov. 2019, 18, 273–294. [Google Scholar] [CrossRef]
  120. Imura, Y.; Nishida, M.; Ogawa, Y.; Takakura, Y.; Matsuzaki, K. Action mechanism of tachyplesin I and effects of PEGylation. Biochim. Biophys. Acta Biomembr. 2007, 1768, 1160–1169. [Google Scholar] [CrossRef] [Green Version]
  121. Kaur, N.; Dilawari, R.; Kaur, A.; Sahni, G.; Rishi, P. Recombinant expression, purification and PEGylation of Paneth cell peptide (cryptdin-2) with value added attributes against Staphylococcus aureus. Sci. Rep. 2020, 10, 1–14. [Google Scholar] [CrossRef] [PubMed]
  122. Makadia, H.K.; Siegel, S.J. Poly Lactic-co-Glycolic Acid (PLGA) as biodegradable controlled drug delivery carrier. Polymers 2011, 3, 1377–1397. [Google Scholar] [CrossRef] [PubMed]
  123. Kumar, P.; Shenoi, R.A.; Lai, B.F.L.; Nguyen, M.; Kizhakkedathu, J.N.; Straus, S. Conjugation of Aurein 2.2 to HPG Yields an Antimicrobial with Better Properties. Biomacromolecules 2015, 16, 913–923. [Google Scholar] [CrossRef] [PubMed]
  124. Almaaytah, A.; Mohammed, G.K.; Abualhaijaa, A.; Al-Balas, Q. Development of novel ultrashort antimicrobial peptide nanoparticles with potent antimicrobial and antibiofilm activities against multidrug-resistant bacteria. Drug Des. Dev. Ther. 2017, 11, 3159–3170. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  125. Sahariah, P.; Sørensen, K.K.; Hjálmarsdóttir, M.; Sigurjónsson, E.; Jensen, K.J.; Másson, M.; Thygesen, M.B. Antimicrobial peptide shows enhanced activity and reduced toxicity upon grafting to chitosan polymers. Chem. Commun. 2015, 51, 11611–11614. [Google Scholar] [CrossRef]
  126. Hou, Z.; Shankar, Y.V.; Liu, Y.; Ding, F.; Subramanion, J.L.; Ravikumar, V.; Zamudio-Vázquez, R.; Keogh, D.; Lim, H.; Tay, M.Y.F.; et al. Nanoparticles of Short Cationic Peptidopolysaccharide Self-Assembled by Hydrogen Bonding with Antibacterial Effect against Multidrug-Resistant Bacteria. ACS Appl. Mater. Interfaces 2017, 9, 38288–38303. [Google Scholar] [CrossRef]
  127. Piras, A.M.; Emaisetta, G.; Esandreschi, S.; Egazzarri, M.; Ebartoli, C.; Grassi, L.; Eesin, S.; Chiellini, F.; Ebatoni, G. Chitosan nanoparticles loaded with the antimicrobial peptide temporin B exert a long-term antibacterial activity in vitro against clinical isolates of Staphylococcus epidermidis. Front. Microbiol. 2015, 6, 372. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  128. Petrin, T.H.C.; Fadel, V.; Martins, D.B.; Dias, S.A.; Cruz, A.; Sergio, L.M.; Arcisio-Miranda, M.; Castanho, M.A.R.B.; Cabrera, M.P.D.S. Synthesis and Characterization of Peptide-Chitosan Conjugates (PepChis) with Lipid Bilayer Affinity and Antibacterial Activity. Biomacromolecules 2019, 20, 2743–2753. [Google Scholar] [CrossRef]
  129. Lee, H.; Lim, S.I.; Shin, S.-H.; Lim, Y.; Koh, J.W.; Yang, S. Conjugation of Cell-Penetrating Peptides to Antimicrobial Peptides Enhances Antibacterial Activity. ACS Omega 2019, 4, 15694–15701. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  130. Ho, P.L.; Ong, H.K.; Teo, J.; Ow, D.S.W.; Chao, S.H. HEXIM1 peptide exhibits antimicrobial activity against antibiotic resistant bacteria through guidance of cell penetrating peptide. Front. Microbiol. 2019, 10, 1–10. [Google Scholar] [CrossRef] [Green Version]
  131. Lehar, S.M.; Pillow, T.; Xu, M.; Staben, L.; Kajihara, K.K.; Vandlen, R.; De Palatis, L.; Raab, H.; Hazenbos, W.L.; Morisaki, J.H.; et al. Novel antibody-antibiotic conjugate eliminates intracellular S. aureus. Nature 2015, 527, 323–328. [Google Scholar] [CrossRef]
  132. Mela, I.; Endo, M.; Sugiyama, H.; Henderson, R.M.; Kaminski, C.F. DNA Origami as a Tool in the Targeted Destruction of Bacteria. Biophys. J. 2019, 116, 324a. [Google Scholar] [CrossRef] [Green Version]
  133. Obuobi, S.; Tay, H.K.-L.; Tram, N.D.T.; Selvarajan, V.; Khara, J.S.; Wang, Y.; Ee, P.L.R. Facile and efficient encapsulation of antimicrobial peptides via crosslinked DNA nanostructures and their application in wound therapy. J. Control. Release 2019, 313, 120–130. [Google Scholar] [CrossRef]
  134. Dijksteel, G.S.; Ulrich, M.M.W.; Middelkoop, E.; Boekema, B.K.H.L. Review: Lessons Learned from Clinical Trials Using Antimicrobial Peptides (AMPs). Front. Microbiol. 2021, 12, 616979. [Google Scholar] [CrossRef] [PubMed]
Ijms 22 11172 g001 550
Figure 1. Structures of (a) Gram-negative bacterial cell walls; (b) Gram-positive bacterial cell walls; and (c) mammalian cell membranes.
Figure 1. Structures of (a) Gram-negative bacterial cell walls; (b) Gram-positive bacterial cell walls; and (c) mammalian cell membranes.
Ijms 22 11172 g001
Ijms 22 11172 g002 550
Figure 2. Mechanisms of acquired antibiotic resistance by bacteria. Drug represented as a dark blue sphere.
Figure 2. Mechanisms of acquired antibiotic resistance by bacteria. Drug represented as a dark blue sphere.
Ijms 22 11172 g002
Ijms 22 11172 g003 550
Figure 3. Mechanisms of action of HDPs: (a) direct killing of the bacteria, (b) immunomodulation. In (a), as indicated on the left, HDPs can translocate through the bacterial membrane to reach inner targets, such as (i) DNA, (ii) RNA or (iii) interfere with biosynthetic reactions by binding to proteins or substrates. The inset schematically shows peptidoglycan biosynthesis in S. aureus. HDPs can interfere at different points in this pathway. In (a), on the right, direct killing through membrane perturbation is shown. The specific mechanisms here are: (iv) barrel stave, (v) toroidal or (vi) carpet or detergent-like pore formation, which lead to cell lysis. In (b), intracellular uptake occurs either through G protein-coupled receptors (GPCRs) (yellow) or direct translocation [40]. Once inside, HDPs can function in a myriad of ways: (i) wound healing, (ii) recruitment and polarization of T cells, (iii) promotion of neutrophil extracellular trap (NET) release, (iv) differentiation of dendritic cells, (v) phagocytosis, (vi) modulation of the host microbiome, (vii) induction of chemokines (blue), which leads to the recruitment of monocytes (grey) and macrophages (purple), (viii) neutralization of lipopolysaccharide (LPS), (ix) induction of anti-inflammatory cytokines and (x) suppression of LPS-induced pro-inflammatory cytokines.
Figure 3. Mechanisms of action of HDPs: (a) direct killing of the bacteria, (b) immunomodulation. In (a), as indicated on the left, HDPs can translocate through the bacterial membrane to reach inner targets, such as (i) DNA, (ii) RNA or (iii) interfere with biosynthetic reactions by binding to proteins or substrates. The inset schematically shows peptidoglycan biosynthesis in S. aureus. HDPs can interfere at different points in this pathway. In (a), on the right, direct killing through membrane perturbation is shown. The specific mechanisms here are: (iv) barrel stave, (v) toroidal or (vi) carpet or detergent-like pore formation, which lead to cell lysis. In (b), intracellular uptake occurs either through G protein-coupled receptors (GPCRs) (yellow) or direct translocation [40]. Once inside, HDPs can function in a myriad of ways: (i) wound healing, (ii) recruitment and polarization of T cells, (iii) promotion of neutrophil extracellular trap (NET) release, (iv) differentiation of dendritic cells, (v) phagocytosis, (vi) modulation of the host microbiome, (vii) induction of chemokines (blue), which leads to the recruitment of monocytes (grey) and macrophages (purple), (viii) neutralization of lipopolysaccharide (LPS), (ix) induction of anti-inflammatory cytokines and (x) suppression of LPS-induced pro-inflammatory cytokines.
Ijms 22 11172 g003
Ijms 22 11172 g004 550
Figure 4. Helical wheel representations (left) of (a) aurein 2.2, (b) peptide 73 and (c) cG4L73. Wheels are generated using https://heliquest.ipmc.cnrs.fr/cgi-bin/ComputParams.py and assume that the peptides adopt a completely α-helical conformation. The mean hydrophobic moment (<μH>) is also given, as is the net charge (note: all the peptides have an amidated C-terminus). On the right is representative data, which illustrates the mechanism of action of each of the peptides: (a) aurein 2.2 causes selective leakage of potassium ions, as measured using a pyranine-based in vitro ion translocation assay; (b) peptide 73 affects peptidoglycan biosynthesis, leading to an accumulation of UDP-MurNAc-peptapeptide, similar to vancomycin (VAN); (c) cG4L73 and its PEG conjugate result in a significant reduction in TNF-α release by LPS-stimulated macrophages (* p ≤ 0.05; *** p ≤ 0.001; **** p ≤ 0.0001 by one-way ANOVA with Dunnett’s multiple comparisons test).
Figure 4. Helical wheel representations (left) of (a) aurein 2.2, (b) peptide 73 and (c) cG4L73. Wheels are generated using https://heliquest.ipmc.cnrs.fr/cgi-bin/ComputParams.py and assume that the peptides adopt a completely α-helical conformation. The mean hydrophobic moment (<μH>) is also given, as is the net charge (note: all the peptides have an amidated C-terminus). On the right is representative data, which illustrates the mechanism of action of each of the peptides: (a) aurein 2.2 causes selective leakage of potassium ions, as measured using a pyranine-based in vitro ion translocation assay; (b) peptide 73 affects peptidoglycan biosynthesis, leading to an accumulation of UDP-MurNAc-peptapeptide, similar to vancomycin (VAN); (c) cG4L73 and its PEG conjugate result in a significant reduction in TNF-α release by LPS-stimulated macrophages (* p ≤ 0.05; *** p ≤ 0.001; **** p ≤ 0.0001 by one-way ANOVA with Dunnett’s multiple comparisons test).
Ijms 22 11172 g004
Table
Table 1. Resistance Mechanisms to HDPs for Gram-negative and Gram-positive pathogens. For extensive details on the mechanisms, the reader is invited to consult the excellent reviews of Mookherjee et al. [40] and Joo et al. [30].
Table 1. Resistance Mechanisms to HDPs for Gram-negative and Gram-positive pathogens. For extensive details on the mechanisms, the reader is invited to consult the excellent reviews of Mookherjee et al. [40] and Joo et al. [30].
MechanismGram-NegativeGram-Positive
protease degradationmetalloproteinases (e.g., ZapA, ZmpA, ZmpB); aspartate proteases (e.g., OmpT, PgtE, Pla)metalloproteinases (e.g.,
aureolysin, SepA); serine
endopeptidases (e.g., V8);
cysteine proteases (e.g., SpeB)
sequestrationextracellular proteins;
biofilm matrix (e.g., alginate, polysialic acid)		extracellular proteins;
biofilm matrix (e.g., poly-N-acetyl glucosamine; poly-gamma-glutamic acid)
surface modificationlipid A phosphate modification; lipid A acylation; O-antigen of LPSd-alanylation of teichoic acids (TA, Figure 1); l-rhamnosylation of WTA; lipid II modification
membrane modificationphosphatidyl glycerol (PG)
acylation		PG amino-acylation
efflux pumpsRND familyABC transporters
Publisher’s Note: MDPI stays neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Share and Cite

MDPI and ACS Style

Drayton, M.; Deisinger, J.P.; Ludwig, K.C.; Raheem, N.; Müller, A.; Schneider, T.; Straus, S.K. Host Defense Peptides: Dual Antimicrobial and Immunomodulatory Action. Int. J. Mol. Sci. 2021, 22, 11172. https://doi.org/10.3390/ijms222011172

AMA Style

Drayton M, Deisinger JP, Ludwig KC, Raheem N, Müller A, Schneider T, Straus SK. Host Defense Peptides: Dual Antimicrobial and Immunomodulatory Action. International Journal of Molecular Sciences. 2021; 22(20):11172. https://doi.org/10.3390/ijms222011172

Chicago/Turabian Style

Drayton, Matthew, Julia P. Deisinger, Kevin C. Ludwig, Nigare Raheem, Anna Müller, Tanja Schneider, and Suzana K. Straus. 2021. "Host Defense Peptides: Dual Antimicrobial and Immunomodulatory Action" International Journal of Molecular Sciences 22, no. 20: 11172. https://doi.org/10.3390/ijms222011172

Note that from the first issue of 2016, this journal uses article numbers instead of page numbers. See further details here.

Article Metrics

Back to TopTop