Hybrid derivative of cathelicidin and human beta defensin-2 against Gram-positive bacteria: A novel approach for the treatment of bacterial keratitis.

Bacterial keratitis (BK) is a major cause of corneal blindness globally. This study aimed to develop a novel class of antimicrobial therapy, based on human-derived hybrid host defense peptides (HyHDPs), for treating BK. HyHDPs were rationally designed through combination of functional amino acids in parent HDPs, including LL-37 and human beta-defensin (HBD)-1 to -3. Minimal inhibitory concentrations (MICs) and time-kill kinetics assay were performed to determine the concentration- and time-dependent antimicrobial activity and cytotoxicity was evaluated against human corneal epithelial cells and erythrocytes. In vivo safety and efficacy of the most promising peptide was examined in the corneal wound healing and Staphylococcus aureus (ATCC SA29213) keratitis murine models, respectively. A second-generation HyHDP (CaD23), based on rational hybridization of the middle residues of LL-37 and C-terminal of HBD-2, was developed and was shown to demonstrate good efficacy against methicillin-sensitive and methicillin-resistant S. aureus [MIC = 12.5-25.0 μg/ml (5.2-10.4 μM)] and S. epidermidis [MIC = 12.5 μg/ml (5.2 μM)], and moderate efficacy against P. aeruginosa [MIC = 25-50 μg/ml (10.4-20.8 μM)]. CaD23 (at 25 μg/ml or 2× MIC) killed all the bacteria within 30 min, which was 8 times faster than amikacin (25 μg/ml or 20× MIC). After 10 consecutive passages, S. aureus (ATCC SA29213) did not develop any antimicrobial resistance (AMR) against CaD23 whereas it developed significant AMR (i.e. a 32-fold increase in MIC) against amikacin, a commonly used treatment for BK. Pre-clinical murine studies showed that CaD23 (0.5 mg/ml) achieved a median reduction of S. aureus bioburden by 94% (or 1.2 log10 CFU/ml) while not impeding corneal epithelial wound healing. In conclusion, rational hybridization of human-derived HDPs has led to generation of a potentially efficacious and safe topical antimicrobial agent for treating Gram-positive BK, with no/minimal risk of developing AMR.

Introduction

Infectious keratitis (IK) represents a major cause of corneal blindness worldwide, with an incidence ranging from 2.5 to 799 per 100,000 population-year[1,2]. It is a common, yet potentially sight-threatening, ophthalmic emergency that often warrants hospital admission for intensive antibiotic treatment and monitoring. IK can be caused by a wide array of microorganisms, including bacteria, fungi, protozoa and viruses. Among all, bacterial keratitis (BK) has been shown to be the main cause for IK in many developed countries, including the US and the UK (> 90% cases), with Staphylococci spp. (30–60%) and Pseudomonas aeruginosa (10–25%) being the two most common bacteria reported[1,3-7]. In view of the diverse causative microorganisms, intensive broad-spectrum topical antibiotics are often administered during the initial treatment of IK. In refractory cases of IK, adjuvant therapy such as photoactivated chromophore-corneal cross-linking (PACK-CXL), amniotic membrane transplant, and therapeutic keratoplasty, are often warranted[8-11].

The current management of IK is challenged by several factors, including the low culture yield[1,2], polymicrobial infection[12,13], and emerging trend of antimicrobial resistance (AMR)[1,14,15]. In the Antibiotic Resistance Monitoring in Ocular Microorganisms (ARMOR) 10-year prospective study, it was shown that 35–50% of the Staphylococci spp. were methicillin-resistant, with ~ 75% of them being multidrug resistant (i.e. resistant to ≥ 3 antibiotic classes)[5]. More compellingly, the increased level of AMR of the causative microorganism has been shown to negatively influence the corneal healing time and final visual outcome[16,17]. Furthermore, complications such as corneal melt, perforation and endophthalmitis may ensue despite timely and intensive antibiotic treatment, necessitating eye-saving surgeries such as tectonic keratoplasty[11,18,19]. All these issues highlight an unmet need for new antimicrobial treatment for IK, particularly that no new class of antibiotic has been discovered since 1987[20].

Host defense peptides (HDPs), or previously known as antimicrobial peptides (AMPs), play vital roles in the innate immune system[21,22]. They are a group of evolutionary conserved small molecules that are ubiquitously expressed by the immune cells and the front-line defense structures, including the ocular surface (OS)[23,24]. They have recently shown promise as potential therapeutic agents due to their broad-spectrum antimicrobial properties with minimal risk of developing AMR[25]. These molecules are usually highly cationic and amphiphilic, with 30–50% of hydrophobicity. The cationic amino acid residues (i.e. lysine and arginine) facilitate the binding of HDPs onto the anionic bacterial membrane (via electrostatic interaction), while the hydrophobic residues interact with the lipid tail region of the membrane, culminating in membrane disruption, leakage of cytoplasmic contents and subsequent cell death[26].

Previous studies have demonstrated that numerous HDPs, including LL-37, human beta-defensin (HBD)-2 and -3, are expressed at the OS and upregulated during IK[23,27-31]. HBD-9, on the other hand, was shown to be downregulated during IK[32]. In addition, it was demonstrated that the modulated levels of HBD-3 and HBD-9 on OS during BK returned to normal baseline following complete healing of ulcers[33]. Furthermore, HDPs exhibit moderate in vitro antimicrobial activity [minimum inhibitory concentration (MIC) of around 50–100 μg/mL) against common ocular surface pathogenic isolates such as S. aureus and P. aeruginosa[34,35], highlighting their essential functions in human OS defense.

Despite their promising potential as effective antimicrobial therapies, several issues have impeded the successful translation of HDPs to clinical use. These include their complex structure–activity relationship (SAR), susceptibility to host/bacterial proteases, physiological conditions, and toxicity to host tissues, amongst others[25,36,37]. In view of these issues, a number of novel strategies, including residue substitution, chemical modification, and hybridization, have been proposed to enhance the therapeutic potential of HDPs[25,36,37].

A number of hybrid peptides, including cecropin A-melittin[38], cecropin A-LL37[39], melittin-protamine[40,41], amongst others[25], have been previously designed and reported in the literature. When compared to the parent peptide, these hybrid peptides demonstrated improved antimicrobial efficacy and/or reduced toxicity to host tissues. However, strategies in combining two human-derived HDPs from two different classes (e.g. LL-37 and HBD) have not been previously explored. In this study, we aimed to develop novel topical antimicrobial treatment for BK using hybridized HDPs derived from different combination of LL-37 and HBD-1 to -3, which are all important HDPs expressed at the OS. The in vivo efficacy and safety of the most promising molecule, CaD23 (a hybrid derivative of LL-37 and HBD-2), was further examined and validated in murine corneal wound healing and S. aureus keratitis models.

Results

In vitro antimicrobial efficacy of HDPs

A total of 12 synthetic HDPs were rationally designed and synthesized based on the templates of native LL-37 and HBD-1 to -3 (Table 1). The MIC values (in μg/ml and μM) of all the tested antibiotics, single and hybrid peptides, in the absence and presence of 150 mM NaCl are summarized in Table 2.

Table 1

Summary of the native and synthetic host defense peptide (HDP) sequences.

Types	Peptides	Peptide sequence	Number of AA	Molecular weight, g/mol	Net charge	Hydrophobicity, <H>	Hydrophobic moment, <µH>
Native	HBD1	DHYNCVSSGG QCLYSACPIF TKIQGTCYRG KAKCCK	36	3934.6	+ 4	0.431	0.348
	HBD2	GIGDPVTCLK SGAICHPVFC PRRYKQIGTC GLPGTKCCKK P	41	4334.2	+ 6	0.489	0.246
	HBD3	GIINTLQKYY CRVRGGRCAV LSCLPKEEQI GKCSTRGRKC CRRKK	45	5161.2	+ 11	0.228	0.097
	LL37	LLGDFFRKSK EKIGKEFKRI VQRIKDFLRN LVPRTES	37	4493.3	+ 6	0.201	0.521
Synthetic single HDPs	Ca12	KRIVQRIKDF LR	12	1571.9	+ 4	0.193	0.782
	BD2a	KCCKKP	6	705.9	+ 3	–	–
	BD3	RGRKCCRRKK	10	1290.6	+ 7	− 0.393	0.300
1st generation HyHDPs	DD12	RGKAKCCKGT KCCKKP	16	1739.2	+ 7	0.031	0.144
	DD13	RGKAKCCKRG RKCCRRKK	18	2165.7	+ 11	− 0.251	0.200
	DD32	RGRKCCRRKK KCCKKP	16	1978.5	+ 10	− 0.194	0.201
	CaD1	KRIVQRIKDF LRRGKAK	17	2112.6	+ 7	− 0.022	0.383
	CaD2	KRIVQRIKDF LRKCCKKP	18	2259.8	+ 7	0.174	0.445
	CaD3	RIKDFLRNGR KCCRRKK	17	2177.7	+ 8	− 0.118	0.234
2nd generation HyHDPs	CaD21	KRIVQRIKDF LRKACKKP	18	2227.8	+ 7	0.106	0.443
	CaD22	KRIVQRIKDW LRKCCKKP	18	2298.9	+ 7	0.200	0.456
	CaD23	KRIVQRIKDW LRKLCKKW	18	2398.0	+ 7	0.294	0.456

Calculation of the physicochemical properties of the peptides was performed using PepCalc (https://pepcalc.com/) and HeliQuest (https://heliquest.ipmc.cnrs.fr/cgi-bin/ComputParams.py).

HBD: human beta-defensin; AA: amino acids; HyHDPs: hybrid host defense peptides; C: cysteine; D: aspartic acid; E: glutamic acid; F: phenylalanine; G: glycine; I: isoleucine; K: lysine; L: leucine; N: aspargine; P: proline; Q: glutamine; R: arginine; S: serine; T: theorine; V: valine; W: tryptophan.

aThe sequence is too short for calculation of hydrophobicity and hydrophobic moment.

Table 2

A summary of the minimum inhibitory concentrations (MICs) of various antibiotics and synthetic human-derived hybrid host defense peptides.

Class of agent	Agents μg/ml (μM)	S. aureus SH1000		S. aureus ATCC 29213		MRSA-OS		MRSA ATCC 43300		S. epidermidis ATCC 12228		P. aeruginosa PAO1-L		P. aeruginosa PA-OS
		0 mM	150 mM	0 mM	150 mM	0 mM	150 mM	0 mM	150 mM	0 mM	150 mM	0 mM	150 mM	0 mM	150 mM
Antibiotics	Amikacin	1.25 (2.13)	2.5 (4.27)	–	–	10 (17.1)	10 (17.1)	–	–	–	–	0.63 (1.08)	1.25 (2.13)	0.63 (1.08)	1.25 (2.13)
	Levofloxacin	0.31 (0.86)	0.31 (0.86)	–	–	0.31 (0.86)	0.31 (0.86)	–	–	–	–	0.31 (0.86)	0.31 (0.86)	0.31 (0.86)	0.31 (0.86)
Full-length peptide	LL37	25 (5.6)	–	–	–	25 (5.6)	–	–	–	–	–	50 (11.1)	–	–	–
	HBD2	100 (23.1)	–	–	–	100 (23.1)	–	–	–	–	–	100 (23.1)	–	–	–
	HBD3	100 (19.4)	–	–	–	100 (19.4)	–	–	–	–	–	100 (19.4)	–	–	–
Single linear HDPs	Ca12	> 200 (> 127.2)	–	–	–	> 200 (> 127.2)	–	–	–	–	–	200 (127.2)	–	–	–
	BD2-6	> 200 (> 283.3)	–	–	–	> 200 (> 283.3)	–	–	–	–	–	> 200 (> 283.3)	–	–	–
	BD3-10	> 200 (> 154.9)				> 200 (> 154.9)						> 200 (> 154.9)		–	–
First–generation hybrid HDPs	DD12	> 200 (> 115)	–	–	–	> 200 (> 115)	–	–	–	–	–	> 200 (> 115)	–	–	–
	DD13	> 200 (> 92.3)	–	–	–	> 200 (> 92.3)	–	–	–	–	–	> 200 (> 92.3)	–	–	–
	DD32	> 200 (> 101)	–	–	–	> 200 (> 101)	–	–	–	–	–	> 200 (> 101)	–	–	–
	CaD1	> 200 (> 94.7)	–	–	–	> 200 (> 94.7)	–	–	–	–	–	> 200 (> 94.7)	–	–	–
	CaD2	> 200 (> 88.5)	–	–	–	> 200 (> 88.5)	–	–	–	–	–	> 200 (> 88.5)	–	–	–
	CaD3	> 200 (> 91.8)	–	–	–	> 200 (> 91.8)	–	–	–	–	–	> 200 (> 91.8)	–	–	–
Second–generation hybrid HDPs	CaD21	200 (89.8)	–	–	–	> 200 (> 89.8)	–	–	–	–	–	100 (44.9)	100 (44.9)	200 (89.8)	–
	CaD22	100 (43.5)	> 200 (> 87.0)	–	–	> 200 (> 87.0)	–	–	–	–	–	200 (87.0)	–	200 (87.0)	–
	CaD23	12.5 (5.2)	25 (10.4)	25 (10.4)	50 (20.8)	25 (10.4)	100 (41.7)	25 (10.4)	100 (41.7)	12.5 (5.2)	12.5 (5.2)	50 (20.8)	50 (20.8)	25 (10.4)	50 (20.8)

All experiments were performed in full-strength cationic Muller-Hinton broth (i.e. MHB-2) and in the absence or presence of physiological tear salt concentration (150 mM NaCl). The MIC values are presented in μg/ml (and μM in bracket). When the MIC level was ≥ 200 μg/ml in the absence of salt, the peptide was not subjected to testing in the presence of salt.

MIC refers to the lowest concentration of antibiotic/peptide that prevents any visible bacterial growth after 24 h of incubation with treatment. Data represent the mean of two biological duplicate from two to three independent experiments.

ATCC: American Type Culture Collection; MRSA-OS: methicillin-resistant S. aureus; OS: ocular surface.

For reference and comparison purposes, the antimicrobial efficacy of the full-length sequence of LL-37 and HBD2 and HBD3 was first determined, though extensive examination was not performed in view of the lack of translational potential for clinical use (due to the cost of synthesis associated with long length of the peptides). LL-37 demonstrated moderate-to-good efficacy against methicillin-sensitive S. aureus [MSSA; MIC = 25.0 μg/ml], methicillin-resistant S. aureus [MRSA; MIC = 25 μg/ml] and P. aeruginosa PAO1-L (MIC = 50 μg/ml) whereas HBD2 and HBD3 exhibited low efficacy (MIC = 100 μg/ml) against all three organisms. Subsequently, the efficacy of the three truncated versions of peptides (6–12 amino acids; based on the native template of HBD-2, HBD-3 and LL-37) and 6 first-generation hybrid HDPs (based on different combinations of LL-37, and HBD-1 to -3) were examined. All of them did not demonstrate any significant antimicrobial efficacy (MIC ≥ 200 μg/ml) against either Gram-positive or Gram-negative bacteria. Further 3s-generation peptides (derived from CaD2 sequence) were synthesized through rational modification: (1) CaD21: substitution of cysteine with alanine; (2) CaD22: substitution of phenylalanine with tryptophan (to increase hydrophobicity); and (3) CaD23: substitution of phenylalanine and proline with tryptophan (to further enhance hydrophobicity) and substitution of cysteine with leucine. CaD21 and CaD22 demonstrated slight improvement in the antimicrobial efficacy whereas CaD23 exhibited good antimicrobial efficacy against MSSA (MIC = 12.5–25.0 μg/ml), (MRSA; MIC = 25 μg/ml) and methicillin-sensitive Staphylococcus epidermidis [MSSE; MIC = 12.5 μg/ml], highlighting the importance of increased hydrophobicity for antimicrobial efficacy (Table 1). Moderate efficacy of CaD23 was observed against P. aeruginosa (MIC = 25–50 μg/ml). When tested in the presence of physiological tear salt concentration (150 mM NaCl), the MIC of CaD23 against MSSA and MRSA increased by two to fourfold, remained unchanged for MSSE, and remained relatively stable (one to twofold increase) against P aeruginosa.

In vitro cell viability and cytotoxicity

Amikacin and CaD2 did not demonstrate any lethal effect on HCE-2 cell viability at 200 μg/ml (Fig. 1A). The IC50 (concentration that inhibits 50% of the cell viability) of CaD21, CaD22 and CaD23 were > 200 μg/ml, > 200 μg/ml and 54.6 ± 11.7 μg/ml, respectively. This demonstrated that the increased hydrophobicity with tryptophan residues enhanced the antimicrobial efficacy of CaD23 but with increased negative effect on the cell viability of HCE-2 cells. In terms of cytotoxicity, amikacin and CaD2 did not show any sign of toxicity for HCE-2 cells at 200 μg/ml and CaD23 showed 30.4 ± 7.8% cytotoxicity at 200 μg/ml (Fig. 1B). The LC50 (concentration that kills 50% of the cells) of CaD23 was > 200 μg/ml, which yielded a therapeutic index (defined by LC50 divided by the MIC value) of > 8 for treating S. aureus ATCC29213. Hemolytic assay demonstrated minimal (7.1 ± 3.0%) hemolytic activity of CaD23 at 200 μg/ml (Fig. 2). A summary of the cell viability, cytotoxicity and hemolytic results of CaD23 is provided in Table 3. In addition, a summary of the therapeutic index of CaD23 (defined as IC50, LC50 or HC50 divided by the MIC value) is provided in Table 4.

Figure 1

Cytotoxicity of synthetic peptides and amikacin (a commonly used antibiotic for bacterial keratitis) in various concentrations against human corneal epithelial cells (HCE-2), presented as dose–response curves (normalized, variable slope). Percentage cell viability is presented as mean ± standard deviation (depicted in error bars) of two independent experiments performed in biological duplicate. Some error bars are missing due to small standard deviation values. (A) Cell viability assay (using cell counting kit-8 assay) demonstrating normal metabolic activity of epithelial cells in CaD2 and amikacin but reduced activity in CaD23 (IC50 = 54.6 ± 11.7 μg/ml) after 3 h of treatment. IC50 (concentration of treatment inhibiting 50% of cell viability) is shown in a black dotted line. (B) Cytotoxicity assay (using lactate dehydrogenase assay) demonstrating no sign of cytotoxicity of epithelial cells in amikacin and CaD2, and low level of cytotoxicity in CaD23 (30.4 ± 7.8% at 200 μg/ml; LC50 > 200 μg/ml) after 3 h of treatment.

Figure 2

Hemolytic effect of CaD23 and levofloxacin (a commonly used antibiotic for bacterial keratitis) in various concentrations against fresh human erythrocytes, determined after 1 h of treatment. Percentage hemolysis is presented as mean ± standard deviation (depicted in error bars) of two independent experiments performed in biological duplicate. Some error bars are missing due to small standard deviation values. The graph demonstrating minimal hemolytic effect of CaD23 against fresh human erythrocytes (only 7.1 ± 3.0% at 200 μg/ml).

Table 3

Summary of the cytotoxicity, cell viability and hemolytic results of antibiotics and synthetic peptides (in µg/ml concentration).

Types	Agents	LC50	Lmax (%)	IC50	Imax (%)	HC50	Hmax (%)
Antibiotics	Amikacin	> 200	0.0 (0.1)	> 200	100.1 (7.3)	> 200	0.0
	Levofloxacin	> 200	1.2 (0.7)	> 200	108.0 (2.8)	> 200	0 (0.0)
First-generation peptides	DD12	–	–	–	–	–	–
	DD13	–	–	–	–	–	–
	DD32	–	–	–	–	–	–
	CaD1	–	–	–	–	–	–
	CaD2	> 200	2.9 (2.2)	> 200	1.9 (7.3)	–	–
	CaD3	–	–	–	–	–	–
Second-generation peptides	CaD21	–	–	> 200	43.9 (1.0)	–	–
	CaD22	–	–	> 200	34.3 (8.2)	–	–
	CaD23	> 200	26.6 (6.5)	54.6 (11.7)	69.6 (7.8)	> 200	7.1 (3.0)

The cytotoxicity and cell viability results were obtained after 3 h of treatment whereas hemolytic effect of treatment was examined after 1 h of treatment.

Results are presented in mean (SD) of two independent experiments performed in biological duplicate. Toxicity results of some peptides were missing because their antimicrobial efficacy was poor and hence toxicity was not determined.

LC50: concentration of treatment causing 50% cytotoxicity; Lmax (%): percentage of cytotoxicity at 200 µg/ml treatment concentration; IC50: concentration of treatment causing 50% inhibition of cell viability; Imax (%): percentage of inhibition of cell viability at 200 µg/ml treatment concentration; HC50: concentration of treatment causing 50% hemolysis; Hmax (%): percentage of hemolysis at 200 µg/ml treatment concentration.

Table 4

Summary of therapeutic index of CaD23 determined based on cytotoxicity, cell viability, and hemolytic results.

μg/ml	S. aureusSH1000		S. aureusATCC29213		MRSA-OS		MRSAATCC43300		S. epidermidisATCC12228		P. aeruginosa PA01-L		P. aeruginosaPA-OS
	MIC	TI	MIC	TI	MIC	TI	MIC	TI	MIC	TI	MIC	TI	MIC	TI
Based on LC50 (= > 200)	12.5	> 16	25	> 8	25	> 8	50	> 4	12.5	> 16	50	> 4	25	> 8
Based on IC50 (= 55)	12.5	4.4	25	2.2	25	2.2	50	1.1	12.5	4.4	50	1.1	25	2.2
Based on HC50 (= > 200)	12.5	> 16	25	> 8	25	> 8	50	> 4	12.5	> 16	50	> 4	25	> 8

The minimum inhibitory concentration (MIC) values, based on the results in the presence of full-strength cationic Muller-Hinton broth (caMHB) without salt, and therapeutic index (TI) values are presented in mean values.

MRSA: methicillin-resistant Staphylococcus aureus; OS: ocular surface (clinical isolate); LC50: concentration of treatment causing 50% cytotoxicity; IC50: concentration of treatment causing 50% inhibition of cell viability; HC50: concentration of treatment causing 50% hemolysis.

Time-kill kinetics

Time- and concentration-dependent antimicrobial activity of CaD23 was determined against MSSA (SH1000) using time-kill kinetics assay. When CaD23 was used at 2× MIC (25 μg/ml) against SH1000, it was able to achieve significant killing (99.9% or 3 log10 CFU/ml reduction) with 15 min and complete killing (100%) within 30 min of treatment (Fig. 3). In contrast, amikacin (used at 20× MIC; 25 μg/ml) could only achieve significant and/or complete killing (99.9–100%) of SH1000 within 4 h of treatment, which was 8 times slower than CaD23. The antimicrobial efficacy of CaD23 (25 μg/ml) and amikacin (both 10 μg/ml and 25 μg/ml) were maintained at 24 h’ time-point, with no evidence of bacterial re-growth. Similar findings were observed when CaD23 and amikacin were tested against SH1000 in physiological tear salt concentration (150 mM NaCl). CaD23 (100 μg/ml; 4× MIC) was able to achieve complete killing of S. aureus within 15 min of treatment whereas amikacin (20 μg/ml; 8× MIC) was only able to achieve complete killing within 4 h of treatment (Fig. 4).

Figure 3

Time-kill kinetics of CaD23 (0.25× MIC and 2× MIC) amikacin (8× and 20× MIC) against S. aureus (SH1000) in cation-adjusted Muller-Hinton broth over 24 h. Phosphate buffer solution (PBS) group serves as the untreated control. “0 min” represents the starting inoculum, which is around 6 log10 CFU/ml. The red dotted horizontal line at 3 log10 CFU/ml signifies the threshold of significant bacterial killing (defined as 99.9% or 3 log10 CFU/ml reduction of the bacterial viability compared to the starting inoculum). Data is presented as mean ± standard deviation (depicted in error bars) of two independent experiments performed in biological duplicate. CaD23 (2× MIC) was able to achieve complete (100%) killing of SH1000 within 30 min of treatment whereas amikacin (8× MIC and 25× MIC) was only able to achieve complete killing of SH1000 within 4 h of treatment. The antimicrobial efficacy of CaD23 and amikacin was maintained at 24 h post-treatment.

Figure 4

Time-kill kinetics of CaD23 (4× MIC) and amikacin (8× MIC) against S. aureus (SH1000) in cation-adjusted Muller-Hinton broth and physiological tear salt concentration (150 mM NaCl) over 24 h. Phosphate buffer solution (PBS) group serves as the untreated control. “0 min” represents the starting inoculum, which is around 6 log10 CFU/ml. The red dotted horizontal line at ~ 3 log10 CFU/ml signifies the threshold of significant bacterial killing (defined as 99.9% or 3 log10 CFU/ml reduction of the bacterial viability compared to the starting inoculum). Data is presented as mean ± standard deviation (depicted in error bars) of two independent experiments performed in biological duplicate. CaD23 (4× MIC) was able to achieve complete (100%) killing of SH1000 within 15 min of treatment whereas amikacin (8× MIC) was only able to achieve complete killing of SH1000 within 4 h of treatment. The antimicrobial efficacy of CaD23 and amikacin was maintained at 24 h post-treatment.

Multipassage antimicrobial resistance (AMR) study

Multipassage AMR assays were performed to evaluate the risk of development of AMR of S. aureus ATCC SA29213 against CaD23 and amikacin over 10 consecutive passages (days). S. aureus did not develop any AMR against CaD23 after 10 consecutive passages whereas it developed significant AMR against amikacin, with a fourfold increase in the MIC after the 2nd passage and a 32-fold increase in the MIC after the 10th passage (Fig. 5). This highlights the therapeutic potential of CaD23 as novel antimicrobial agent in the era of emerging AMR.

Figure 5

Multipassage antimicrobial resistance (AMR) assays for CaD23 and amikacin against S. aureus ATCC SA29213 over 10 consecutive passages (days). S. aureus did not develop any AMR against CaD23 after 10 passages whereas it developed significant AMR against amikacin, with a fourfold increase in the MIC after the 2nd passage and a 32-fold increase in the MIC after the 10th passage. Data is presented as mean ± standard deviation (depicted in error bars) of two independent experiments performed in biological duplicate. Some error bars are missing due to small or no standard deviation values.

In vivo safety of CaD23

In view of the known discrepancy between in vitro and in vivo results, the safety of CaD23 was further determined in a murine corneal epithelial wound healing model. When compared to the PBS group, both CaD23 0.03% (or 300 μg/ml) and CaD23 0.05% (or 500 μg/ml) groups did not show any significant difference in the rate of corneal re-epithelialization (all healed within 2–3 days), suggesting that both concentrations were safe for topical application (Fig. 6). However, significant delay in corneal re-epithelialization was observed in the CaD23 0.1% group, with a mean wound size of 28.5 ± 19.9% at day 3 post-injury (p = 0.004).

Figure 6

In vivo safety of CaD23 in various concentrations [0.03% (or 300 μg/ml), 0.05% (or 500 μg/ml), and 0.1% (1 mg/ml)] and phosphate buffer solution (PBS) assessed in a murine corneal epithelial wound healing model (n = 4 mice/treatment group). (A) Representative slit-lamp images showing the daily progress of corneal wound healing of each treatment group. The green color-stained area depicts the corneal epithelial defect. Complete corneal re-epithelialization was observed in all treatment groups, except CaD23 0.1% group, by day 3. The images were analyzed using ImageJ software (https://imagej.nih.gov/ij/)[67]. (B) Graphical summary of the progress of corneal re-epithelialization of each treatment group over 3 days. The corneal epithelial wound size at various time points is calculated based on the original 100% wound size at baseline. Data is presented as mean ± standard deviation.

In vivo efficacy of CaD23

Based on the in vivo safety results, the highest tolerable concentration of CaD23 0.05% was subjected to subsequent in vivo efficacy testing in a murine S. aureus ATCC 29213 keratitis model. As the data was not normally distributed and was log-transformed, the results were reported in median ± interquartile range (IQR). When compared to the S. aureus bacterial viability in the PBS group (4.2 ± 1.3 log10 CFU/ml), there was a considerable reduction of bacterial viability in the CaD23 0.05% and levofloxacin 0.5% groups by 94% (3.0 ± 2.4 log10 CFU/ml; p = 0.72) and 98% (2.4 ± 2.2 log10 CFU/ml; p = 0.08), respectively, though statistical significance was not achieved due to wide standard deviations (Fig. 7). At day 3 post-treatment, the clinical appearance of the corneas in the CaD23-treated group (1.2 ± 0.45; p = 0.07) and the levofloxacin-treated group (1.0 ± 0.71; p = 0.03) was substantially better than the untreated group (2.2 ± 0.84), based on the ocular clinical scoring (Fig. 7).

Figure 7

In vivo efficacy of CaD23 0.05% (500 μg/ml), levofloxacin 0.5% (positive control) and phosphate buffer solution (PBS; negative control) in a murine S. aureus ATCC SA29213 bacterial keratitis model (n = 5 mice/treatment group). (A) Representative slit-lamp images showing the corneal appearance over 3 days post-infection in each treatment group. Note the significant infiltrative changes of cornea in the PBS group as compared to the CaD23 0.05% and levofloxacin 0.5% groups. (B) Scatter plot showing the bacterial viability of S. aureus (in log10 CFU/ml) after 3 days of treatment. In view of the wide range of results, data is presented as median ± interquartile range. (C) Scatter plot showing the ocular clinical scoring of the clinical appearance of the S. aureus-infected corneas treated by different treatment. The data is presented as median ± interquartile range. The scores are interpreted as follows: 0: Clear cornea or minimal opacity, partially covering the pupil; (b) + 1: Mild opacity, partially/fully covering the pupil; (c) + 2: Dense opacity, partially covering the pupil; (d) + 3: Dense opacity fully covering the pupil; and (e) + 4: Corneal perforation or phthisis.

Discussion

IK represents a persistent and uncurbed burden on human health at a global level. Topical antibiotics are the current mainstay of treatment for BK but the efficacy is being increasingly challenged by the emergence of AMR[1,2,14]. In addition, patients with BK often require long duration of treatment and sight-threatening complications may still ensue despite timely intervention[11], highlighting an unmet need for newer and better treatment. HDPs serve as an attractive class of antibiotics for treating IK based on the following reasons: (1) the broad-spectrum activity of HDPs can provide comprehensive coverage to a wide range of microorganisms, particularly when mixed infection is relatively common (5–20%) in IK[1]; (2) the rapid antimicrobial action help reduce the microbial load and limit the damage to the cornea more effectively, ultimately have a better chance of preserving the vision, as well as reducing the risk of developing AMR, which is currently an emerging issue in ocular infection[14]; and (3) HDPs can be used as synergistic or additive agents to the current conventional antibiotics, enhancing the therapeutic index by increasing the antimicrobial efficacy and reducing the dose-related toxicity[42,43].

In this study, we highlight a body of work in designing and developing human-derived hybrid HDP as topical treatment for BK. Hybridization strategy has been previously employed by several research groups to improve the therapeutic index of HDPs[39,40,44] but the strategy of using human-derived hybrid HDPs (with LL-37 and HBD-2) is first of its kind. The initial concept of developing synthetic HDPs derived from LL-37 and HBD was founded on the observation of the upregulation of these key HDPs at the ocular surface during IK[23,27,33,45]. Furthermore, LL-37 and HBD-2 and -3 were shown to exhibit good antimicrobial efficacy against a range of organisms[34,45]. We have selected the mid-region of LL-37, consisting of residues 18–29 of LL-37 (i.e. KR-12) as part of the hybrid template as studies have demonstrated that KR-12, though much shorter than parent LL-37, exhibited similar antimicrobial activity against E. coli (MIC =  ~ 64 μg/ml) with reduced toxicity to host cells[46]. C-terminal of HBD1-3 was used as the other part of the hybrid template in view of its rich content of cationic residues, which have been shown to play an important role in interacting with anionic bacterial membrane and killing of bacteria[47,48].

Our initial attempt of engineering single linear HDPs (including LL-37 and HBD-2 and -3) and hybrid HDPs (based on LL-37 and HBD-1 to -3) did not yield any compound with good antimicrobial efficacy. However, with systematic SAR analysis and modification, particularly through substitution of proline and phenylalanine with tryptophan residues (to increase hydrophobicity and membrane partitioning), ensued the development of peptide with enhanced antimicrobial efficacy against MSSA (MIC = 12.5–25 μg/ml) and MRSA (MIC = 25 μg/ml), serving as a proof-of-concept of this novel design strategy. Interestingly, increased hydrophobicity augmented the antimicrobial activity of HDP against Gram-positive bacteria more than Gram-negative bacteria. This is likely attributed to the different compositions in the bacterial membrane between Gram-positive bacteria, which consist of a thick peptidoglycan layer, and Gram-negative bacteria, which comprises an additional outer membrane with abundance of negatively charged lipopolysaccharide for which cationicity of the peptide plays a more important role[49]. In addition, the efficacy of CaD23 (18 amino acids in length) is at least equal to or stronger than the full-length parent LL37 (MIC = 25–50 μg/ml), HBD-2 (MIC = 100 μg/ml) and HBD-3 peptides (MIC = 50–100 μg/ml). Peptides with shorter sequence not only have the advantage of lower manufacturing cost but may also have a lower risk of inducing immunogenicity[25,50]. Moreover, the antimicrobial efficacy of CaD23 is comparable to some of the HDPs that are developed for ocular surface infection, including esculentin-1a (1–21)NH2[51], RP444[52], melimine and its derivatives[40,53], and ε-lysylated Mel-4[54].

In the time-kill kinetics study, we demonstrated that CaD23 at 2× MIC was able to achieve complete killing of S. aureus within 30 min as compared to 4 h with amikacin at 20× MIC (i.e. 8 times slower than CaD23). We also observed that increasing the concentration of amikacin from 8× MIC to 20× MIC did not expedite its anti-bacterial action against S. aureus, suggesting that the speed of bacterial killing is more related to the underlying mechanism of action than the concentration of antibiotic. The rapid killing action of CaD23 is likely related to a membrane perturbation effect[55], which is in contrast to amikacin where it exerts its anti-bacterial activity via intracellular inhibition of the 30S subunit of bacterial ribosome[56]. The rapid and membrane disruptive action of CaD23 is likely accountable for the low risk of S. aureus developing AMR against CaD23 as the bacteria has less time to adapt and require substantial modification of genome to develop effective resistant mechanisms, which are shown in conventional antibiotics such as amikacin.

Based on the LDH cytotoxicity assay, CaD23 was shown to be relatively non-cytotoxic (20–30% toxicity) at 200 μg/ml, with a therapeutic index of > 8–16 against S. aureus (defined by LC50 concentration divided by MIC value). In addition, the hemolytic activity of CaD23 at 200 μg/ml was only less than 10%. Interestingly, the IC50 value (based on cell viability assay) was around 50 μg/ml, considerably lower than the LC50 value. This discrepancy may be due to the fact that some of the cells were metabolically inhibited but the cell membrane was not disrupted, therefore the IC50 value was lower than the LC50 value. That said, our in vivo corneal epithelial wound healing study showed that CaD23 did not demonstrate any significant toxicity when used at 500 μg/ml (or 0.05%), which was 10 times higher than the IC50 value. The observed discrepancy between in vitro and in vivo findings is likely attributed to the inherent dynamic environment of ocular surface with eye blinking, high tears turnover, and drainage, and dilution of the peptide by the tears[57]. This also suggests that in vitro plate-based static assays such as cytotoxicity or cell viability assays could potentially overestimate the in vivo cytotoxicity of drugs that are developed for ocular topical application. The shortcoming of in vitro assays may be addressed by the recently developed novel ex vivo biomimetic model where it could simulate the dynamic and complex interface between the ocular surface and the external environment, allowing a better prediction of the in vivo effect[58].

Our in vivo BK study demonstrated that CaD23 0.05% (20× MIC) was able to reduce the bacterial viability of S. aureus by 94% when compared to the untreated control group, which was more than the pre-defined endpoint of the study (i.e. 1 logCFU or 90% reduction in the bacterial bioburden). However, the effect was not statistically significant due to the considerably wide standard deviation observed in both the treatment and the control groups. This similarly explained the insignificant improvement in the levofloxacin-treated group, though there was 1.8 logCFU median reduction in the bacterial bioburden compared to the PBS group. Nevertheless, these results serve as a strong proof-of-concept that CaD23 may be employed as a potentially efficacious treatment for treating Gram-positive bacterial keratitis, but a larger sample size will be required to fully ascertain its efficacy. In addition, we had chosen to sacrifice the mice at day-3 post-infection because S. aureus keratitis had been shown to be most severe in C57BL/6J mice at 3-day post-infection, as compared to other stains of mice such as BALB/c and A/J mice. In addition, S. aureus keratitis has been shown to improve spontaneously in C57BL/6J mice at day-5 post-infection and beyond[59]. To investigate the longer-term in vivo antimicrobial efficacy of CaD23 in S. aureus keratitis, other strains of mice may be required to examine this aspect.

One potential approach to improve the therapeutic effect of HDP-derived antimicrobial treatment is to use them in combination with antibiotics as peptide-antibiotic synergism has been demonstrated in several studies[42,43,60]. This attractive antimicrobial strategy not only helps extend the lifespan and broaden the antibacterial spectrum of conventional antibiotics, but also reduce the dose-dependent toxicity associated with HDPs and antibiotics[61]. Recently, our group has also shown that FK16, a cathelicidin-derived molecule, could improve the antimicrobial efficacy of vancomycin, a glycopeptide antibiotic, against PA by eightfold[42]. This is likely ascribed to the different mechanisms of action between FK16 and vancomycin where the membrane disruptive action of FK16 facilitates the diffusion of vancomycin across the bacterial membrane. Hence, future work investigating the potential synergism between CaD23 and commonly used antibiotics for BK would be useful.

At present, our aim is to develop the human-derived hybrid HDPs as topical treatment for BK. However, it is interesting to note that the hemolytic activity of CaD23 was very low (7.1% at 200 μg/ml), suggesting that it can potentially be developed for treating systemic infection. It also reduces the concern of systemic toxicity when it is applied to the ocular surface because systemic absorption of ocular topical treatment can occur, particularly when the drugs are hydrophobic[57]. The considerable disparity between the hemolytic activity and cytotoxicity against corneal epithelial cells could be attributed to the difference in the membrane structure (particularly the cytoskeleton) and the metabolic structures of the non-nucleated cells (e.g. red blood cells) and nucleated cells (e.g. corneal epithelial cells)[62]. Further studies examining the efficacy and stability of CaD23 in serum as well as its interaction with blood proteins will be conducted to determine its therapeutic potential for treating systemic infection.

In conclusion, we demonstrated that rational hybridization of LL-37 and HBD-2 serves as a useful strategy in translating the therapeutic potential of human-derived HDPs. Future work examining the efficacy and safety of combined CaD23-antibiotic therapy would be beneficial. Potential strategies such as N- and C-terminal modifications, introduction of unnatural amino acids and nanoformulation of CaD23 will be further explored with an aim to enhance the antimicrobial efficacy, reduce the toxicity and improve the stability of the peptide[25].

Materials and methods

The commercially synthesized peptides and commonly used antibiotics for IK were first examined for their in vitro antimicrobial efficacy against a range of bacteria. In vitro cytotoxicity of these antimicrobial agents was then determined against human corneal epithelial cells (HCE-2, CRL-11135, ATCC, UK) using cell viability assay and cytotoxicity assay, and against human erythrocytes using hemolytic assay. The most promising synthetic peptide, CaD23, was further examined for its time- and concentration-dependent in vitro antimicrobial activity. Finally, in vivo efficacy and safety of CaD23 were evaluated in corneal wound healing and S. aureus keratitis murine models. All the assays described in this study were conducted in biological duplicate and in at least two independent experiments, with appropriate positive controls (PCs) and negative controls (NCs). Continuous values were expressed in mean ± standard deviation (SD), unless specified otherwise.

Design and synthesis of HDPs

A template-based design method was used to design our human-derived HDPs. The native peptide sequences were obtained from an established protein bank database (https://www.uniprot.org/). Several human-derived HDPs, specifically HBD-1, -2, and -3, and cathelicidin (LL-37), were subject to testing and hybridization. The physicochemical properties of the designed peptides, including peptide weight, net charge, hydrophobicity (), and amphiphilicity/hydrophobic moment (<μH>, were analyzed using a computational programmes such as PepCalc (https://pepcalc.com/) and HeliQuest (http://heliquest.ipmc.cnrs.fr). Various strategies, including residue substitution and hybridization, were employed for SAR analysis and for improving the therapeutic index (i.e. increasing the antimicrobial efficacy and reducing the toxicity profile). The native and synthetic peptide sequences are shown in Table 1.

Synthesis of the single and hybrid HDPs was based on the knowledge of the functional regions of the native templates. Three single, short-sequenced (truncated) peptides, based on the native template of HBD2, HBD3 and LL-37, were first generated. Truncated versions of the parent peptides were engineered as this strategy has been shown to serve as a useful method in improving the efficacy of peptides and reducing the cost of synthesis, which represents a significant translational barrier of peptide-based antimicrobial therapy[25]. The C-terminal region of HBD2 and HBD3 was synthesised and examined in view of the presence of high cationicity (i.e. rich of lysine and/or arginine residues), which are important for the antimicrobial efficacy[26,47,48]. In addition, the middle region of LL-37, same as the KR12 molecule, was synthesized as it has been shown to exhibit efficacy equivalent to the full-length of LL-37[46].

All antibiotics, including amikacin (an aminoglycoside) and levofloxacin (a fluoroquinolone), were purchased from Sigma-Aldrich, United Kingdom. Both antibiotics were used as positive controls as they were commonly used for treating BK[1,4,63]. The full-length peptides were commercially produced by Anaspec (Cambridge, UK; for LL-37) and PeproTech (London, UK; for HBD-2 and HBD-3). All other peptides were commercially produced by Mimotopes (Mulgrave Victoria, Australia) via the traditional solid phase Fmoc synthesis method. All the synthetic peptides were purified by reverse-phase high performance liquid chromatography (RP-HPLC) to > 95% purity and characterized by mass spectrometry.

Range of microorganisms being tested

A range of Gram-positive and Gram-negative laboratory- and clinical-strain bacteria were used for the experiments. These included laboratory-strain methicillin-sensitive S. aureus (MSSA; including SH1000 and ATCC SA29213), laboratory-strain MRSA (ATCC MRSA43300), clinical-strain MRSA (MRSA-OS; an IK isolate), laboratory-strain methicillin-sensitive Staphylococcus epidermidis (MSSE; ATCC SE12228), laboratory invasive-strain P. aeruginosa (PAO1-L), and clinical cytotoxic-strain P. aeruginosa (PA-OS; an IK isolate).

Determination of antimicrobial efficacy using MIC assay

In vitro antimicrobial efficacy of the antibiotics and designed HDPs was determined using an established MIC assay with broth microdilution method approved by the Clinical and Laboratory Standards Institute (CLSI)[64]. Briefly, the microorganisms were cultured on Tryptone Soya Agar (TSA) and incubated overnight for 18–21 h at 37 °C. Bacterial inoculums were subsequently prepared using the direct colony suspension method[64]. Three to five bacterial colonies were obtained from the agar plate and inoculated into an Eppendorf tube containing 1 ml of cation-adjusted Muller-Hinton broth (caMHB), consisting of 20–25 mg/L calcium ions (Ca2+) and 10–12.5 mg/L magnesium ions (Mg2+). The bacterial suspension was adjusted to achieve a turbidity equivalent to 0.1 OD600 or 0.5 MacFarland, containing ~ 1.5 × 108 colony-forming unit (CFU)/ml, which was then further diluted in 1:150 in caMHB to reach a final bacterial concentration of ~ 1 × 106 colony forming units (CFU)/ml. Each treatment (peptide or antibiotic) was prepared in 1:2 serial dilution in 96-well polypropylene microplates (with a final treatment volume of 50 μl per well), followed by the addition of 50 μl of 1 × 106 CFU/ml bacteria into each well (with a final bacterial concentration of 5 × 105 CFU/ml). As the HDPs are known to be influenced by the salt content[25], the MIC assay was also performed in the presence of physiological tear salt concentration (150 mM NaCl). The MIC values, defined as the lowest concentration of the antimicrobial agent that prevented any visible growth of bacteria, were determined after 24 h of incubation with treatment.

Cell viability and cytotoxicity assays

Cell viability and cytotoxicity of antibiotics and peptides were determined against human corneal epithelial cells (HCE-2, CRL-11135, ATCC, Manassas, Virginia, USA) using cell-counting-kit-8 (CCK-8) assay (Sigma Aldrich, Merck Life Science UK Limited, Dorset, UK) and lactate dehydrogenase (LDH) assay (ThermoFisher Scientific, UK), respectively, as per manufacturer’s guidelines. HCE-2 cells were cultured and seeded into a 96-well plate at a density of 7.5 × 103 cells/well and allowed to attach overnight and grew to 80–90% confluency in keratinocyte serum free medium (KSFM) supplemented with human recombinant epidermal growth factor, bovine pituitary extract, hydrocortisone, and insulin. Once the confluency reached 80–90%, the cells were incubated with treatment for 3 h before OD450 measurement was taken using BMG Clariostar microplate reader (BMG Labtech Ltd., Aylesbury, UK). Appropriate controls were used, including 0.1% Triton X-100 as positive control and KSFM as negative control. Cell viability was calculated using the following formula: [((Itreatment – INC)/(INC)) × 100; I = intensity] and cytotoxicity was calculated using the following formula: [((Itreatment – INC)/(IPC – INC)) × 100].

Hemolytic assay

Ethical approval was obtained from the Local Research Ethics Committee of University of Nottingham prior to the experiment (Ref: 176-1812). The experiment was conducted in accordance with the relevant guidelines and regulations. Hemolytic assay was performed according to the previously established protocol[42]. Briefly, 5 ml of fresh human blood was collected from healthy participants with written informed consent, in an EDTA tube and centrifuged for 10 min at 1300g at 10 °C for separation of plasma. The remaining erythrocytes were rinsed and centrifuged further three times in Ca2+/Mg2+ free Dulbecco’s phosphate-buffered saline (DPBS). Subsequently, erythrocytes were diluted to 8% v/v in DPBS and incubated with 100 μl of treatment, positive control (1% Triton X-100) and negative control (DPBS), all in 1:1 ratio, for 1 h (final erythrocytes concentration = 4% v/v). After 1 h of incubation, the plate was centrifuged at 500×g for 5 min and 100 μl of supernatant of each well was transferred into a 96-well plate for measurement at OD540. Hemolysis (%) was calculated as [(Itreatment – INC)/(IPC – INC)] × 100.

Time-kill kinetics assay

Time-kill kinetics assay was performed to determine the time-dependent and concentration-dependent in vitro antimicrobial effects of the CaD23 and amikacin, a commonly used topical antibiotics for BK, against 100 μl of ~ 1 × 106 CFU/ml of SH1000 (1:1 treatment-bacteria ratio) at various time points, including 0 min (pre-treatment), 15 min, 30 min, 60 min, 2 h, 4 h, and 24 h. At each time point, 10 μl of the treated bacteria was transferred to an Eppendorf tube containing 90 μl of PBS, which was then serially diluted in 1:10 concentration for inoculation on agar plates and incubated overnight for 18–21 h at 37 °C for enumeration of CFU.

Multipassage AMR assays were performed to evaluate the risk of development of AMR of S. aureus (ATCC SA29213) against CaD23 and amikacin over 10 consecutive passages (days). The assay was conducted in a similar manner of the MIC assay described above. After determining the initial MIC level of each treatment at baseline (passage 1), bacterial suspensions were obtained from the 0.5× MIC well of each treatment and were adjusted in caMHB to achieve a turbidity equivalent to 0.1 OD600 (containing ~ 1.5 × 108 CFU/ml). This was then further diluted in 1:150 in caMHB to reach a final bacterial concentration of ~ 1 × 106 colony forming units (CFU)/ml. Subsequently, 50 μl of 1 × 106 CFU/ml of the bacteria was added to the corresponding serially diluted treatment and the MIC level was determined after 24 h of incubation with treatment. Development of AMR was defined as ≥ fourfold increase in the MIC level compared to the baseline.

In vivo efficacy and safety studies

The in vivo studies were conducted in two stages, namely the corneal wound healing study (for safety) and BK study (for efficacy), based on previously established protocols[54,65]. Wild-type C57BL/6J mice (8–9 weeks old, male, average weight of 25 g) were used in view of the consistent and reproducible results demonstrated in previous studies[54,65]. The mice were maintained and treated in compliance with the Guide for the Care and Use of Laboratory Animals (National Research Council) and the ARVO statement for the Use of Animals in Ophthalmic and Vision Research. All animal studies were conducted at the Singapore Eye Research Institute, Singapore, and were approved by the Animal Welfare & Ethical Review Body (AWERB), University of Nottingham, UK (Ref: UoN-Non-UK #16), the Institutional Animal Care and Use Committee (IACUC) and the Institutional Biosafety Committee (IBC) of SingHealth, Singapore (Ref: 2019/SHS/1491). All experiments were performed in accordance with relevant guidelines and regulations. General anesthesia was administered using intraperitoneal injections of xylazine (10 mg/kg) and ketamine (80 mg/kg)], and a drop of topical proxymetacaine hydrochloride 0.5% was administered immediately before wounding and/or infecting the corneas. Upon completion of the experiments, all mice were sacrificed according to the method of humane killing set out in Animals (Scientific Procedures) Act 1986 Schedule 1 using overdose of general anesthesia via intraperitoneal route. The study was reported in accordance with ARRIVE guidelines (https://arriveguidelines.org)[66].

In vivo corneal wound healing study

Drug drainage, blinking and tear film were considered during dosing translation from in vitro to in vivo use[52]. Based on the MIC of CaD23 against S. aureus ATCC 29213 (= 25 μg/ml), a range of concentration of CaD23 was chosen, including 300 μg/ml (0.03%; 12× MIC), 500 μg/ml (0.05%; 20× MIC) and 1 mg/ml (0.1%; 40× MIC).

In vivo safety of CaD23 (in 0.03%, 0.05% or 0.1%), and PBS (negative control) was first determined in a mouse corneal epithelial wound healing model. In the absence of in vivo pilot data of our designed HDPs, the sample size was calculated based on a previous study[67]. This was designed as a non-inferiority trial to ensure that the HDPs did not affect the wound healing when compared to PBS (control). The non-inferiority margin was set at 10% difference of the wound size between HDPs and PBS at 3 days (deemed as significantly different), with a standard deviation (SD) of 5% (Cohen’s d = 2.0), power = 80% and p < 0.05. A minimum sample size of 4 mice/treatment group was needed.

All mice were randomly allocated to each of the four treatment groups (n = 4 mice/group). Prior to the study, all eyes were examined with slit-lamp biomicroscopy to confirm the health of corneas. Under general and topical anesthesia, the central 2 mm corneal epithelium was gently debrided with sterile Beaver mini-blades, leaving the basal lamina intact. Each treatment was applied immediately after wounding, then 4 times a day at 3-h interval for 3 days (total dose of treatment per mouse = 14). Corneal epithelial defect was assessed using a cobalt-blue filter-equipped slit-lamp biomicroscopy and photography with staining with topical sodium fluorescein 1% at baseline (immediately post-debridement) and daily up to 3 days post-treatment. Fluorescein-stained images of the corneal wound defect were analyzed using ImageJ software (https://imagej.nih.gov/ij/)[68]. The main outcome measure was the wound size at the end of day 1, 2 and 3 [expressed as % of the original wound size in mean and standard deviation (SD)]. Difference in the wound size between groups was analyzed using one-way ANOVA with Dunnett’s post hoc test (PBS as the control group).

In vivo S. aureus keratitis study

Based on the in vivo safety data, the highest tolerable concentration of CaD23, 500 μg/ml (0.05%), was used in the subsequent S. aureus keratitis murine model. Levofloxacin 0.5%, a commonly used antibiotic for BK in clinical setting[4], and PBS were used as the positive and negative controls, respectively. In the absence of in vivo pilot data, the sample size was calculated based on a previous study[65]. To detect an effect size of 1 LogCFU (or 10 times) difference in the bacterial load (significant antimicrobial efficacy) between HDPs (mean = 5 logCFU) and PBS (mean = 6 logCFU; NC), with a SD of 0.5 logCFU (Cohen’s d = 2.0), power = 80% and p < 0.05, a minimum sample size of 4–5 mice/group is required.

All mice were randomly allocated to each treatment group (n = 5 mice/group). Slit-lamp examination was performed before the start of experiment to confirm the health of corneas. Under general and topical anesthesia, the central 2 mm corneal epithelium was gently removed with sterile Beaver mini-blades. 10 μl of ~ 1 × 108 CFU/ml of ATCC SA29213 was applied topically onto the cornea and the lid was held shut for 1 min. At 6 h post-infection, 10 μl of treatment was applied directly onto the infected corneas with a dose regimen of 4 times a day at 3-h interval for 3 days (total dose of treatment per mouse = 12). The eyes were monitored daily using slit-lamp biomicroscopy and photography. Ocular clinical scoring was adapted from a previous method described by Clemens et al.[52] with minor modifications: (a) 0: Clear cornea or minimal opacity, partially covering the pupil; (b) + 1: Mild opacity, partially/fully covering the pupil; (c) + 2: Dense opacity, partially covering the pupil; (d) + 3: Dense opacity fully covering the pupil; and (e) + 4: Corneal perforation or phthisis.

At the end of day 3, all animals were sacrificed, and the infected eyes were enucleated. The whole corneas were subsequently dissected and homogenized in 1 ml of sterile PBS using sterile glass micro-beads. The homogenised infected corneal tissue suspension was serially diluted in 1:10 and plated on TSA plates in triplicates for enumeration of CFU after 24 h incubation at 37 °C. The main outcome measures were the ocular clinical scoring and the residual bacterial load at 3-day post-treatment (expressed as log10 CFU/ml, which was the same as log10 CFU/cornea) and the difference among groups was analyzed using one-way ANOVA with Dunnett’s post hoc test (PBS as the control group).