Background
Wound healing is a complex process involving many cell types and mediators that regulate tissue repair. Successful wound healing and tissue regeneration depends on tightly regulated hemostasis, inflammation, matrix synthesis, proliferation, wound contraction and tissue remodeling to restore tissue function and integrity [
1,
2]. A thermal injury is among the most severe forms of trauma with effects both locally and systemically [
3]. Patients with large burn injuries have a multitude of immunological alterations and impaired functions of multiple effector cells of innate immunity and acquired immunity (including macrophages, dendritic cells (DC), natural killer (NK) cells, and T cells) at the wound site or a systemic change in circulating inflammatory mediators [
3‐
8].
Systemic inflammation can lead to profound suppression of the innate and adaptive immune system [
4‐
8] resulting in increased sepsis, wound healing complications, multi-system organ failure, and remote organ injury at sites such as the lung, liver, small intestines, and brain, representing major causes of morbidity and mortality in burn trauma patients [
3,
9]. These thermally induced organ injuries appear to be caused by toxic inflammatory mediators produced by infiltrating activated neutrophils early after thermal injury that are associated with increased chemokine levels [
10‐
13].
The complex balance between innate and adaptive immune cell function after a severe injury is vital in determining wound healing outcome [
4]. Innate immune cells show a progressive increase in the production of pro-inflammatory immune regulatory molecules (IL-1β, IL-6, TNFα and PGE
2), while cells of the adaptive immune system display counter-inflammatory responses such as IL-10 and TGFβ [
13‐
15]. The interplay between pro- and anti-inflammatory mechanisms is key for avoiding further tissue damage beyond that of the primary insult and a systemic inflammatory response [
4,
6‐
8,
13,
16].
Mice of the MRL/MpJ strain have been reported to have a unique capacity for limited regenerative wound healing, as shown by the complete closure of 2-mm ear-hole wounds [
17‐
19]. Excised tissue is quickly replaced with normal tissue architecture that retains its full functionality. In contrast, others have shown that small, open, excisional cutaneous wounds in MRL/MpJ mice heal with marked scarring and no evidence of tissue regeneration [
17,
20‐
22]. Recently, our laboratory reported that a severe thermal wound on the dorsum of MRL/MpJ mice heal with scar formation and a delay in two critical wound healing events: wound closure and myofibroblast development [
22]. The mechanism(s) involved are unclear, but it appears that the anatomical site of the injury, the severity of the injury, and the milieu of pro- or anti-inflammatory cytokines are all critical factors in determining whether a wound heals with or without a scar [
20,
21,
23‐
25]. Moreover, in the MRL/MpJ mouse model we have demonstrated that the systemic response to a severe thermal injury can trigger a lethal autoimmune response within weeks-to-months following severe traumatic injury [
26]. Understanding the dichotomous role of innate immune responses and inflammation on tissue regeneration versus delayed healing and scar formation may ultimately lead to innovative approaches for treatment of severe wounds to promote accelerated and scarless healing as well as tissue regeneration.
In this study we show in wild-type MRL/MpJ mice that scarless ear-hole healing does not occur following a severe thermal injury at an anatomically remote site. During the early inflammatory phases of healing, we observed marked pathological cutaneous skin lesions on the ear pinnae, including hyperkeratosis, acanthosis, mononuclear cell infiltration and necrosis in close proximity to ear-hole wound margins. In addition, we observed a significantly augmented inflammatory response in the serum, lung, ear wound, and burn wound margin tissue by analyzing various chemokine/cytokine expression levels. These findings underscore the profound importance of the systemic inflammatory response following peripheral tissue injury which can modulate other cellular events critical in wound healing, as evidenced by the impediment of an otherwise normal and complete wound healing-tissue regenerative response in MRL/MpJ mice.
Methods
Animals
Age matched (8-12 weeks) female MRL/MpJ mice were purchased from the Jackson Laboratory (Bar Harbor, ME) and housed at the Walter Reed Army Institute of Research/Naval Medical Research Center (WRAIR/NMRC) animal facility, which is certified by the Association for the Assessment and Accreditation of Laboratory Animal Care International. All procedures were conducted using facilities and protocols approved by the Animal Care and Use Committee of WRAIR (protocols #K06-05 and K01-08). The experiments reported herein were conducted in compliance with the Animal welfare Act and in accordance with the principles set forth in the current edition of the Guide for Care and Use of Laboratory Animals, Institute for Laboratory Animal Resources, National Research Council, National Academy Press, 1996. Animals were housed 5 to a cage until study initiation, and individually housed thereafter using standard micro-isolator polycarbonate caging. Animal rooms were kept at 21 ± 2°C with 50 ± 10% humidity on a 12-hr light/dark cycle. Commercial rodent ration (Harlan Teklad Rodent Diet 8604) was available freely, as was acidified (pH = 2.5) water to control opportunistic infections.
Burn wound model
Mice were anesthetized with an intraperitoneal injection of ketamine (75 mg/kg), xylazine (15 mg/kg), and acepromazine (2.5 mg/kg). After shaving the dorsum, the exposed skin was washed gently with room temperature sterile water and prepped with Betadine (a 10% povidone-iodine solution for skin disinfection). The Betadine solution from the prep area was wiped off using 3 series of sponge gauzes containing 70% isopropyl alcohol. A single full thickness circular burn (15 mm diameter; ~15% total body) was introduced with electrocautery Bovie (370-400°C for 1.5 sec; Bovie Aaron Medical, St. Petersburg, FL) on the mid-dorsum of each mouse. This protocol produces a histologically proven well demarcated, full thickness, anesthetic injury that is non-lethal (< 0.5% mortality). Wounds were treated with bacitracin (Pharmaderm, Melville, NY) (applied topically) immediately after wounding, left uncovered, and allowed to desiccate. Once mice recovered from anesthesia, they were placed alone in separate cages and maintained under standard conditions in the animal facility (as described above). Buprenorphine (Reckitt Benckiser Pharmaceuticals, Richmond, VA) 0.1 mg/kg SC BID was given on post-operative days 1 through 3 for pain management. No additional therapeutic intervention was provided, as administration of anti-inflammatory or analgesic drugs may introduce complications into the assessment of inflammatory responses. Wounds became covered with inflammatory eschar, and no infection was evident macroscopically. At various time points post injury, cohorts of mice were killed by carbon dioxide inhalation and subsequent cervical dislocation. At the time of killing, cardiac blood was collected and serum was obtained and aliquoted and stored at -80°C until use. Lungs and wound edge/margin tissue from the ear and skin were collected and stored in RNALater (Ambion, Austin, TX). All samples were kept at 4°C until use.
Ear wound and ear-hole-closure measurements
A 2-mm through-and-through circular hole was made in the center of the cartilaginous part of each ear using a standard surgical biopsy punch (Acuderm, Inc, Ft. Lauderdale, FL) immediately following thermal injury. Ear-hole diameter size was determined using a 7X Bausch & Lomb ocular magnifier (Fisher Scientific) immediately following the wounding procedure (day 0) and at frequent intervals over a 31-day evaluation period. Mice with ear-holes that were not cleanly cut or altered in configuration by the mice through scratching within a few days of injury were excluded from the study. Typically, in non-injured mice, the circular wounds healed in a circular fashion whereby the mean hole diameter was calculated by taking the average of the longest and the corresponding perpendicular measurement. Wound size was calculated based on the formula A = (d/2)2 (π), where A is the area of the wound in square millimeters and d is the mean ear-hole diameter.
Cytokine and chemokine measurements
Quantification of murine IL-1α, IL-1β, IL-2, IL-3, IL-4, IL-5, IL-6, IL-7, IL-8, IL-10, IL-12(p40), IL-12(p70), IL-13, IL-15, IP-10, Eotaxin, IFN-γ, GM-CSF, MCP-1, MIP-1α, RANTES, TNFα and MIP-2α in mouse serum was determined in duplicative measurements using Luminex-100 technology (Austin, TX) with Fluorokine MAP Multiplex Mouse Cytokine Panels (R&D Systems, Minneapolis, MN) and Mouse Proinflammatory (7-plex) Arrays (Mesoscale Discovery, Gaithersburg, MD) in accordance to manufacturer's instructions. Sample concentrations were interpolated from standard curves, and results were expressed in pg/ml.
Total RNA was extracted from skin, lung and ear tissue and stored in RNALater (Ambion, Austin, TX). Briefly, tissue was homogenized using Trizol reagent (Invitrogen, Carlsbad, CA) and total RNA was isolated using Qiagen RNeasy Lipid Tissue Mini Kit (QIAGEN Inc. Valencia, CA) according to manufacturer's instructions. Sample quantity, and quality was assessed by determining the A260/280, A260/230 ratio on a Nanodrop 2000 Spectrophotometer (NanoDrop Technologies Inc. Wilmington, DE) and by measuring 28S/18S ribosomal RNA ratios and RNA Integrity Number (RIN) using an Agilent 2100 BioAnalyzer (Agilent Technologies Inc., Santa Clara, CA). Agilent RNA integrity values for all sampled wound specimens in this study were ≥ 8.5. Reverse transcription was performed with Roche 1st Strand Synthesis kit (Roche Diagnostics Corporation, Indianapolis, IN). Briefly, 1.0 μg sample RNA was added to a master mix containing 1x reaction buffer, 5 mM MgCl2, 1 mM deoxynucleotide mix, 6.4 μg random primers, 100 units RNase inhibitor, and 40 units AMV reverse transcriptase. 10 mM Tris buffer, pH 7.5 was used to reach 40 μl final reaction volume. Then, final reaction mixture was subjected to a single reverse-transcription cycle of 25°C for 10 min, 42°C for 60 min, 99°C for 5 min, and 4°C for at least 10 min.
Real-Time quantitative PCR (RT-PCR) gene profiling for pro-inflammatory transcripts
Quantitative real-time polymerase chain reaction (RT-PCR) was performed using the ABI Prism 7900 HT Sequence Detection System (Applied Biosystems, Foster City, CA). Custom designed 'Wound Repair' TaqMan® Low Density Array (TLDA) cards (Applied Biosystems, Foster City, CA) and catalogued "Primer Assays" (SABiosciences, Rockville, MD) were used to assess gene expression of a small cohort of pro-inflammatory and/or anti-inflammatory cytokines: (IL-1α, IL-1β, IL-6, TNFα, MCP-1, MIP-2α, IL-10, PGE-2, MIP-1α, MIP-1β, PF-4, ENA-78, IP-10, I-TAC, and iNOS). Amplification parameters were as follows: one cycle of 50°C for 2 min and 95°C for 10 min followed by 40 cycles of 95°C for 30 sec and 60°C for 1 min.
RT-PCR data analysis
RT-PCR data were analyzed using the Sequence Detection System version 2.3 included with the ABI Prism 7900 HT RT-PCR system or using Microsoft Excel. The threshold cycle (C
t) for each sample was manually set to 0.2 and the baseline was set between 3 and 15 cycles. 18 S ribosomal RNA was used as an endogenous housekeeping control for normalization and the comparative C
t method was used to calculate the relative fold expression by
. Assays with C
t values greater than 35 cycles were excluded from analysis [
27,
28].
Statistics
Statistical analysis of variance was used to analyze the data and a nonparametric Mann-Whitney U test was used to determine the level of significance of differences in sample means (GraphPad PRISM 4.0). A p value < 0.05 was considered significant.
Discussion
Numerous studies have shown that severe traumatic injury can lead to systemic pro-inflammatory responses and cellular immune dysfunction [
4‐
8,
12,
13,
16]. In this study, we demonstrate that systemic wound trauma inflammatory signaling, mediated by acute thermal injury, attenuates normal ear-hole closure and scarless healing in MRL/MpJ mice. Based on our previous findings that MRL/MpJ mice exhibit a delay in wound closure and myofibroblast development following sever thermal trauma, and that these mice show a propensity to develop the autoimmune state lupus following significant tissue injury [
22,
26], we hypothesized that the activation of specific cell types and the production of cytokines and other wound healing reparative mediators may be detrimental to a remote ear-hole tissue regenerative response in MRL/MpJ mice following traumatic tissue injury. Several other groups have examined the link between local injury and a systemic response. Similar to our findings Schwacha et al [
29], reported a significant inflammatory response after burn wounds in small animals and delayed wound healing distant to the site of injury.
In the present study, we show attenuated ear-hole closure and tissue regeneration in a large percentage of MRL/MpJ mice following a remote, severe, full-thickness, cutaneous thermal injury. Pathological examinations of ear-hole wounds demonstrated excessive sequestration and infiltration of macrophage and neutrophils. The majority of the MRL/MpJ ear wounds healed with histological evidence of fibrosis and scar formation or became chronically inflamed and necrotic to the point where some of the animals had to be euthanized. The precise reasons for aberrant ear-hole healing (wound closure) in these mice following thermal injury are unclear, but may be related to heightened systemic inflammation, higher fibrotic cytokine signaling and the overproduction of danger signals (presence of pathogens, pathogen-derived molecules, or even self-derived molecular danger signals, which arise from tissue damage) [
30] which lead to uncharacteristic healing and scar formation.
An essential feature of scarless healing/tissue regeneration in adults and in fetal tissues appears to be a diminished cytokine response to injury [
1,
31,
32]. On the other hand, cytokines introduced into the fetal environment evoke heightened inflammatory responses and tissue fibrosis [
33,
34]. Similarly, PGE
2 stimulates leukocyte accumulation, fibroblast proliferation, and collagen deposition resulting in delayed wound healing and scar formation when introduced into early fetal wounds [
35].
Elevated levels of IL1-β, IL-6, TNFα, PGE
2, iNOS and various chemokines are associated with areas of local as well as systemic inflammation [
13]. We observed a heightened inflammatory response at the site of a remote secondary injury following severe burn trauma; a pathological picture suggestive of a global systemic immune response. In contrast, blunted expression and production of IL-1β, IL-6, TNFα, iNOS correlated with complete ear-hole closure and scarless tissue healing. Pathological examinations of ear-hole wounds in thermally injured mice demonstrated excessive sequestration and infiltration of macrophage and neutrophils. These observations lead us to speculate that macrophage hyperactivity after thermal injury may play a critical role in altered ear-hole healing response, as primed hyperactive macrophages might contribute to the increased recruitment and sequestration of leukocytes, tissue inflammation, and damage-tissue necrosis precipitated through excessive cytokine and chemokine production [
36].
Competing interests
The authors declare that they have no competing interests.
Authors' contributions
TAD conceived and designed the research. TAD, MFA, KA and SRZ carried out all the experimental work and data collection. TAD, MFA, KA, EAE and SRZ conducted the data analysis and interpretation. TAD, EAE, and SRZ wrote the manuscript and/or made critical revisions. All authors read and approved the final version of the manuscript.