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Expression and Localization of Cathepsins B, D, and G in Dupuytren’s Disease

Tan, Kirin, MB ChB*; Brasch, Helen, D., BMedSc, MBChB*; van Schaijik, Bede, BTech (Hons)*; Armstrong, James, R., MBBS, MD*†; Marsh, Reginald, W., PhD*‡; Davis, Paul, F., PhD*; Tan, Swee, T., MBBS, PhD*†; Itinteang, Tinte, MBBS, PhD*

Plastic and Reconstructive Surgery – Global Open: February 2018 - Volume 6 - Issue 2 - p e1686
doi: 10.1097/GOX.0000000000001686
Experimental
New Zealand

Background: The pathogenesis of Dupuytren’s disease (DD) remains unclear. An embryonic stem cell (ESC)–like population in the endothelium of the microvessels around tissues that expresses components of the renin-angiotensin system (RAS) has been reported. This study investigated if this primitive population expresses cathepsins B, D, and G, that contribute to RAS bypass loops.

Methods: 3,3-Diaminobenzidine immunohistochemical (IHC) staining for cathepsins B, D, and G was performed on sections of formalin-fixed paraffin-embedded DD cords (n = 10) and nodules (n = 10). Immunofluorescence IHC staining was utilized to demonstrate co-expression of these cathepsins with ESC markers. Protein and gene expression of these cathepsins was investigated in snap-frozen DD cords (n = 3) and nodules (n = 3) by Western blotting and NanoString analysis, respectively. Enzymatic activity of these cathepsins was investigated by enzymatic activity assays.

Results: 3,3-Diaminobenzidine IHC staining demonstrated expression of cathepsins B, D, and G in DD cords and nodules. Gene expression of cathepsins B, D, and G was confirmed by NanoString analysis. Western blotting confirmed expression of cathepsins B and D, but not cathepsin G. Immunofluorescent IHC staining demonstrated high abundance of cathepsins B and D on the OCT4+/angiotensin converting enzyme+ endothelium and the smooth muscle layer of the microvessels. Cathepsin G was localized to trypase+ cells within the stroma in DD cords and nodules with limited expression on the microvessels. Enzyme activity assays demonstrated functional activity of cathepsins B and D.

Conclusions: Cathepsins B, D, and G were expressed in the DD tissues, with cathepsins B and D localized to the primitive population in the endothelium of the microvessels, whereas cathepsin G was localized to phenotypic mast cells, suggesting the presence of bypass loops for the RAS.

From the *Gillies McIndoe Research Institute, Wellington, New Zealand; Wellington Regional Plastic, Maxillofacial & Burns Unit, Hutt Hospital, Wellington, New Zealand; and University of Auckland, Auckland, New Zealand.

Received for publication August 31, 2017; accepted January 5, 2018.

Presented at the New Zealand Association for Plastic Surgeons’ and the Australian and New Zealand Society of Oculoplastic Surgeon’s Joint Annual Scientific Meeting, Queenstown, New Zealand August 4–6, 2017.

Drs. Tan and Itinteang contributed equally to this work.

Disclosure: Drs. Davis, Tan, and Itinteang are inventors of a patent application Treatment of Fibrotic Conditions (no. PCT/NZ2016/050187). The authors have no financial interest to declare in relation to the content of this article. The Article Processing Charge was paid for by the Gillies McIndoe Research Institute general fund.

Supplemental digital content is available for this article. Clickable URL citations appear in the text.

Swee T. Tan, ONZM, MBBS, PhD, FRACS, Gillies McIndoe Research Institute, PO Box 7184, Newtown 6242, Wellington, New Zealand, E-mail: swee.tan@gmri.org.nz

This is an open-access article distributed under the terms of the Creative Commons Attribution-Non Commercial-No Derivatives License 4.0 (CCBY-NC-ND), where it is permissible to download and share the work provided it is properly cited. The work cannot be changed in any way or used commercially without permission from the journal.

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INTRODUCTION

Dupuytren’s disease (DD) is a fibro-proliferative disorder characterized by progressive palmar fascia fibrosis, with a variable prevalence that increases with age, predominantly affecting males of Northern European ancestry.1 , 2 Although the risk factors for DD are well known, its pathogenesis remains unclear.

The development of thick collagenous cords that results in progressive fixed flexion contractures of the digits in DD leads to functional impairment. Management options for DD include steroid injections, collagenase injections and surgery.3 The mainstay treatment of DD is surgery, most commonly fasciectomy, which is associated with recurrence, in up to 70% of patients.4 The absence of an effective treatment for DD is underscored by the incomplete understanding of the pathogenesis of this common condition.3 , 4

Previous studies suggest mesenchymal stem cells (MSCs), which give rise to the proliferating myofibroblasts, are critical in the development of DD.5 , 6 An embryonic stem cell (ESC)–like population within the endothelium of the microvessels surrounding the cords and nodules of DD has been identified.7 This primitive population expresses components of the renin-angiotensin system (RAS), namely pro(renin) receptor, angiotensin converting enzyme (ACE), angiotensin II receptor 1 (ATIIR1) and angiotensin II receptor 2 (ATIIR2).8 These findings suggest that dysfunction of the ESC-like population within the microvessels of DD may give rise to an intermediate MSC population, which in turn gives rise to the abundant downstream myofibroblasts—the dominant cell type within DD.9 A putative role for the RAS in regulating this ESC-like population has been speculated, reminiscent of the findings in infantile hemangioma.10

The availability of ATII, the vasoactive downstream peptide of RAS pathway, may be promoted by cathepsins B, D, and G, proteases that contribute to RAS bypass loops.11 , 12

Cathepsin B, a cysteine protease produced as the inactive pro-cathepsin B, is homologous to renin.11 It converts angiotensinogen (AGN) to ATI13 , 14 and contributes to tumor invasion and metastasis.15 Cathepsin B is also implicated in the development of glioblastoma,16 rheumatoid arthritis,17 and oral tongue squamous cell carcinoma.18 Cathepsin D, an aspartyl protease, produced as the inactive pro-cathepsin D, is a homolog of renin.14 , 15 It converts AGN to ATI14 , 15 and is implicated in the formation of pulmonary19 and renal20 fibrosis. Cathepsin G, a serine proteinase, is converted from inactive pro-cathepsin G.21 , 22 It is homologous to ACE, and it increases the availability of ATII from either AGN or ATI.11 , 12 Stored in neutrophil granules, cathespin G is a proteolytic enzyme involved in immune defense and inflammation.23

In this study, we investigated the expression of cathepsins B, D, and G, and their localization in relation to the ESC-like population within DD7 that expresses components of the RAS,8 using immunohistochemical (IHC) staining, Western blotting (WB), and Nanostring mRNA analysis. We also investigated the function of these enzymes using enzyme activity assays.

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METHODS

Tissue Samples

DD tissue samples from 10 male patients aged 66–78 (mean, 69.3) years including 6 patients used in our previous studies7 , 8 were sourced from the Gillies McIndoe Research Institute Tissue Bank and used for this study that was approved by the Central Regional Health and Disability Ethics Committee (ref. no. 13NTB155). These DD samples were divided into cords and nodules by the operating surgeon (J.R.A.), which were processed for analysis separately. Written consent was obtained from all participants.

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Histochemical and IHC Staining

Hematoxylin and eosin staining was performed on 4-μm-thick formalin-fixed paraffin-embedded sections of DD nodules and cords from 10 patients to confirm the presence of DD by an anatomical pathologist (H.D.B.). These sections underwent 3,3-diaminobenzidine (DAB) IHC staining. Antigen retrieval was performed using sodium citrate (Leica) at 95°C for 15 minutes. All sections underwent single DAB IHC staining with the primary antibodies, cathepsin B (1:1000; cat# sc-6490-R, Santa Cruz, Calif.), cathepsin D (1:200; cat# NCL-CDm, Leica, Wetzlar, Germany), cathepsin G (1:200; cat# sc-33206, Santa Cruz, Calif.), OCT4 (1:200; cat# NBPI-47923, Novus Biologicus, Littleton, Colo.), ACE (1:100; cat# 3C5, AbD Serotec, Oxford, United Kingdom), and tryptase (ready-to-use; cat# PA0019, Leica) with detection using the bond polymer refine detection kit (Leica).

Cords and nodules of 2 representative DD samples from the original cohort of 10 patients included in DAB IHC staining were selected for immunofluorescence (IF) IHC staining with the same primary antibodies at the same concentrations, but using a combination of Vectafluor Excel anti-mouse (ready-to-use; cat# VEDK2488, Vector Laboratories, Burlingame, Calif. or Alexa Fluor anti-rabbit 594 (1:500; cat# A21207, Life Technologies, Carlsbad, Calif.) as appropriate secondary antibodies. All antibodies were diluted in Bond primary antibody diluent (Leica), and all DAB and IF IHC staining were performed on the Leica Bond Rx auto-stainer (Leica, Nussloch, Germany). IF IHC stained slides were mounted using Vectashield hardset medium with DAPI (Vector Laboratories).

Positive controls included human placenta for cathepsin B,24 epidermis of human skin for cathepsin D,25 and mouse bone marrow for cathepsin G.26 Negative controls for DAB IHC staining were performed on sections of DD cords and nodules using a matched isotype control for both mouse (ready-to-use; cat# IR750, Dako, Copenhagen, Denmark) and rabbit (ready-to-use; cat# IR600, Dako) primary antibodies, to determine the specificity of the amplification cascade. Negative controls for IF IHC staining were performed using a section of DD cord and nodule with the combined use of primary isotype mouse (ready-to-use; cat# IR750, Dako) and rabbit (ready-to-use; cat# IR600, Dako) antibodies.

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Image Analysis

DAB IHC-stained slides were viewed and imaged using an Olympus BX53 microscope fitted with an Olympus DP21 digital camera (Olympus, Tokyo, Japan). IF IHC-stained slides were viewed and imaged using an Olympus FV1200 biological confocal laser-scanning microscope and processed with cellSens Dimension 1.11 software using 2D deconvolution algorithm (Olympus).

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WB

Total protein was extracted from snap-frozen samples of DD cords and nodules from 3 of the original cohort of 10 patients used for DAB IHC staining, by pestle homogenization (cat# PES-15-B-SI, Corning, N.Y.) in ice-cold Radioimmunoprecipitation assay buffer buffer (cat# R0278, Sigma-Aldrich, St. Louis, Mass.) supplemented with 1× HALT protease and phosphatase inhibitor cocktail (cat# 78440, Pierce Biotechnology, Rockford, Ill.) and 10 mM dithiothreitol (cat# 43816, Sigma-Aldrich). Soluble proteins were precipitated with ProteoExtract Protein Precipitation Kit (cat# 539180, Merck Millipore, Billerica, Mass.) and then resuspended at 70°C in Bolt 1× lithium dodecyl sulfate sample buffer (reduced sample) (cat# B0007, Thermo Fisher Scientific, Waltham, Mass.) at -20°C for 1 hour. Equal amounts of protein (~30 μg total protein per sample) were heated at 70oC and resolved by 4–12% 1D-PAGE (cat# NW04120BOX, Thermo Fisher Scientific) and transferred to a polyvinylidene fluoride membrane (cat# IB24001, Invitrogen, Carlsbad, Calif.) using an iBlot 2 (cat# IB21001, Thermo Fisher Scientific). Blotted membranes were blocked using 10 mL of 1× iBind Flex FD solution (cat# SLF2019, Thermo Fisher Scientific) for 5 minutes at room temperature and probed using the iBind Flex device (cat# SLF2000, Thermo Fisher Scientific) for cathepsin B (1:250; cat# SC-6490-R, Santa Cruz), cathepsin D (1:250; cat# SC-6486, Santa Cruz), cathepsin G (1:250; cat# ab197354, Abcam, Cambridge, United Kingdom), and β-actin (1:500; cat# ab8226 and ab8229, Abcam). Appropriate secondary antibodies were goat anti- rabbit Alexa Fluor 647 (1:2000; cat# A21244, Life Technologies) for cathepsins B and D, chicken anti-goat Alexa Fluor 647 (1:2000; cat# A21469, Life Technologies) for β-actin ab8229, goat anti-mouse Alexa Fluor 488 (1:2000; cat# A21202, Life Technologies) for β-actin ab8226, and goat anti-rabbit horseradish peroxidase (1:2000; cat# ab6721, Abcam) for cathepsin G. Clarity Western ECL (cat# 1705061, Bio-Rad) was used as the substrate for visualizing horseradish peroxidase detected protein bands and the Chemi Doc MP Imaging System (Bio-Rad) and Image Lab 5.0 software (Bio-Rad) were used for band detection and analysis. All experiments were performed in triplicate. Snap-frozen tonsillar tissue was used as control tissue for cathepsin B27 and cathepsin D28 and a recombinant cathepsin G protein (cat# H00001511-Q01, Novus Biologicals, Littleton, Colo.) was used as an appropriate positive control. Matched mouse (1:500; cat# ab18443, Abcam) and rabbit (1:500; cat# ab171870, Abcam) isotype controls were used as appropriate negative controls.

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Enzymatic Activity Assay

Enzymatic activities of cathepsin B and cathepsin D were determined in snap-frozen DD cords and nodules from the same 3 patients used in the WB, using enzymatic activity assay kits for cathepsin B (cat# ab65300; Abcam) and cathepsin D (cat# ab65302; Abcam). All steps of the procedure were performed according to the manufacturer’s protocol. Fluorescence was measured in a Nunc F96 MicroWell black polystyrene plate (cat# 136101, Thermo Fisher Scientific) using the Varioskan Flash plate reader (cat# MIB5250030, Thermo Fisher Scientific). Tonsil and denatured tonsil tissue lysates were used as appropriate positive and negative controls, respectively.

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Nanostring MRNA Analysis

Snap-frozen samples of DD cords and nodules from the same 3 patients subjected to WB and enzymatic activity assays were used to isolate total RNA for NanoString nCounter Gene Expression Assay (NanoString Technologies, Seattle, Wash.). RNA was extracted from frozen tissues using RNeasy Mini Kit (Qiagen) and subjected to the NanoString nCounter gene expression assay by New Zealand Genomics Ltd (Dunedin, New Zealand). The probes for the genes encoding cathepsin B (CTSB; NM_001908.3), cathepsin D (CTSD; NM_001909.3), cathepsin G (CTSG; NM_001911.2), and the housekeeping gene GUSB (NM_00181.3) were used. Raw data were analyzed by nSolver software (NanoString Technologies) using standard settings and were normalized against the housekeeping gene.

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Statistical Methods

GraphPad (QuickCalcs) software for t test was used to analyze the NanoString data.

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Ethics Approval

Central Regional Health and Disability Ethics Committee (ref. no. 13NTB155).

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RESULTS

Histochemical and DAB IHC Staining

DAB IHC staining demonstrated expression of cathepsin B (Supplemental Digital Content 1 A and B, brown), cathepsin D (Supplemental Digital Content 1 C and D, brown) and cathepsin G (Supplemental Digital Content 1 E and F, brown) in DD cords (Supplemental Digital Content 1 A, C, and E) and nodules (Supplemental Digital Content 1 B, D, and F). Cathepsin B and cathepsin D were localized to the endothelium and the smooth muscle layer of the microvessels [see figure, Supplemental Digital Content 1, which displays representative DAB IHC-stained sections of DD cords (A, C, and E) and DD nodules (B, D, and F), http://links.lww.com/PRSGO/A682]. Expression of cathepsin G was primarily localized to a small number of cells within the stroma with limited expression on the endothelium and smooth muscle of the microvessels. There was no observable difference in the expression of each cathepsin in the DD cords and nodules.

Positive controls for cathepsins B, D, and G demonstrated appropriate staining in human placenta (Supplemental Digital Content 2A, brown), epidermis of human skin (Supplemental Digital Content 2, brown), and mouse bone marrow (Supplemental Digital Content 2C, brown), respectively. The negative control demonstrated minimal staining [Supplemental Digital Content 2D, brown; see figure, Supplemental Digital Content 2, which displays positive controls of DAB IHC staining for cathepsin B (A, brown), cathepsin D (B, brown), and cathepsin G (C, brown) demonstrated on sections of human placenta, epidermis of human skin and mouse bone marrow, respectively, http://links.lww.com/PRSGO/A683].

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IF IHC Staining

IF IHC staining was performed to determine the localization of each cathepsin in relation to the ESC-like population within DD tissue7 that expresses the components of the RAS.8 Cathepsin B (Fig. 1A, D, red) and cathepsin D (Fig. 1B, E, red) but not cathepsin G (Fig. 1C, F, red) were expressed by the OCT4+ ESC-like population (Fig. 1A–F, green) on the endothelium of the microvessels in DD cords (Fig. 1A–C) and DD nodules (Fig. 1D–F). Cathepsin G (Fig. 1C, red) was localized to the OCT4+ (Fig. 1C, green) cells located within the stroma, away from the microvessels in both the DD cords (Fig. 1C) and DD nodules (Fig. 1F). Cathepsin B (Fig. 2A, D, red) and cathepsin D (Fig. 2B, E, red), but not cathepsin G (Fig. 2C, F, red) were expressed by the ACE+ (Fig. 2A–F, green) endothelium, in both DD cords (Fig. 2A–C) and DD nodules (Fig. 2D–F). Cathepsin G (Fig. 2G, H, red) was localized to cells within the stroma that expressed tryptase (Fig. 2G, H, green) in both DD cords (Fig. 2G) and DD nodules (Fig. 2H), similar to the phenotypic mast cells in infantile hemangioma.10

Fig. 1

Fig. 1

Fig. 2

Fig. 2

Split images in Figure 1 and Figure 2 are shown in Supplemental Digital Content 3 and Supplemental Digital Content 4, respectively (see figure, Supplemental Digital Content 3, which displays split images of IF IHC-stained images shown in Fig. 2A–F, http://links.lww.com/PRSGO/A680; see figure, Supplemental Digital Content 4, which displays split images of IF IHC-stained images shown in Fig. 3A–H, http://links.lww.com/PRSGO/A681). The negative controls for IF IHC staining demonstrated minimal staining in a DD cord (Supplemental Digital Content 4Q) and a DD nodule (Supplemental Digital Content 4R), as expected.

Fig. 3

Fig. 3

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Nanostring MRNA Analysis

NanoString mRNA analysis for cathepsins B, D, and G, normalized against the housekeeping gene GUSB, confirmed transcriptional activation for all the aforementioned genes in both DD cords and nodules (Fig. 3). The average expression of cathepsin B, in both DD cords and nodules, was significantly greater than that of cathepsin D (P = 0.02), and the average expression of cathepsin D was significantly greater than that of cathepsin G (P = 0.004).

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WB

WB of the snap-frozen samples of DD cord (n = 3) and nodule (n = 3) demonstrated the presence of bands at the expected molecular weight for cathepsin B (Fig. 4A) and cathepsin D (Fig. 4B). Cathepsin B was detected at the appropriate molecular weight of 25 kDa31 in all 3 DD nodule samples and 2 out of 3 DD cord samples. Cathepsin D was detected at 28 kDa35 in all 3 DD nodule samples and 3 DD cord samples. Cathepsin G was not detected in any of the DD tissue samples at the expected molecular weight of 29 kDa36 (Fig. 4C), with specificity of the antibody confirmed in the positive control, which demonstrated detection of a band at the expected molecular weight of 37 kDa, consistent with the supplier’s product information. β-actin (Fig. 4A–C) confirmed equivalent protein loading for all 3 DD cord and nodule samples examined.

Fig. 4

Fig. 4

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Enzymatic Activity Assays

To determine the functional activity of both cathepsin B and cathepsin D, which were detected by WB, we performed enzymatic activity analysis on the same snap-frozen DD tissue samples, for both cathepsins. All DD cord and nodule samples demonstrated enzymatic activity of cathepsin B and cathepsin D relative to that of the positive and negative control tissues (Fig. 5).

Fig. 5

Fig. 5

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DISCUSSION

Previous studies suggest MSCs may give rise to the proliferating myofibroblasts, a hallmark of fibrosis, characteristic of DD.5 , 6 A putative upstream ESC-like population within DD tissue7 has been demonstrated, and it has been suggested that this primitive population may give rise to the MSCs previously identified.5 This ESC-like population expresses components of the RAS: pro(renin) receptor, ACE, ATIIR1, and ATIIR2, suggesting a crucial role for the RAS in the pathogenesis of DD.8 To the best of our knowledge, this is the first study that demonstrates the expression of cathepsins B, D, and G in both DD cords and nodules.

Cathepsins B, D, and G are proteases that contribute to bypass loops of the RAS (Fig. 6). Cathepsin B that converts pro-renin to renin, is synthesized as pro-cathepsin B, an inactive pro-enzyme, with a molecular weight of 37–39 kDa.29 , 30 Pro-cathepsin B is activated by endogenous aspartic proteinases, or through autocatalysis in acidic conditions (pH, 4.5–5.5)30 , 32 and is subsequently converted to cathepsin B, which consists of a 30 kDa single chain and a 25–26 kDa heavy chain doublet.33 , 34

Fig. 6

Fig. 6

Similarly, cathepsin D converts AGN to ATI, and it is initially produced as pro-cathepsin D with a molecular weight of 52 kDa. Pro-cathepsin D is then converted in the endoplasmic reticulum by renin or pH-dependent autocatalysis, resulting in the mature form of cathepsin D, consisting of a 28 kDa heavy chain and a 14 kDa light chain.35

Cathepsin G converts AGN to ATI or ATII and is produced from a precursor pro-cathepsin G, with a molecular weight of 32.5 kDa. Pro-cathepsin G is converted to active cathepsin G of 29–30 kDa, by the proteolytic activity of cathepsin C.36

The expression of cathepsins B, D, and G demonstrated by IHC staining was confirmed by NanoString mRNA analysis. We have also shown significantly higher transcript expression of cathepsin B than cathepsin D, with both being significantly more abundant than that of cathepsin G.

The protein expression of cathepsin B and cathepsin D was also confirmed by WB and enzymatic activity assays demonstrated functional activity of these cathepsins. IHC staining demonstrated expression and localization of cathepsin G to very few cells within DD cords and nodules. It is therefore not surprising that cathepsin G was below detectable levels by WB.

IF IHC staining demonstrated that cathepsin B and cathepsin D were expressed by the ESC-like population within the endothelium of the microvessels that expresses the ESC marker OCT4, and ACE, a component of the RAS. We infer that these cathepsins may provide bypass loops for the RAS, thus increasing the availability of ATII.

Mast cells have been shown to be overexpressed in DD tissue suggesting a role in this condition.37 The demonstration of expression of cathepsin G by the OCT4+ mast cells within the DD cords and nodules is novel, similar to the observation in proliferating infantile hemangioma.10 Cathepsin G, along with other proteases, is released from mast cells following stimulation by agents such as substance P.37 Apart from contributions to a bypass loop in the RAS, cathepsin G possesses other actions38 although its precise role in DD remains unclear.

The expression of components of the RAS by the ESC-like population in the microvessels within DD tissue8 suggests a crucial role of the RAS in the regulation of the primitive population, which may then differentiate into the mesenchymal progenitors, through an endothelial-to-mesenchymal transition.39 , 40 This ESC-like population may be a novel therapeutic target through modulation of the RAS using existing medications. This hypothesis is supported by the observation of improvement in fibrotic conditions, such as keloid scar, following administration of low-dose enalapril, an ACE inhibitor.41 , 42

In conclusion, we have demonstrated that cathepsin B and cathepsin D are abundantly expressed by the ESC-like population in the endothelium of the microvessels surrounding DD cords and nodules, and that these cathepsins are functionally active. We have also shown that cathepsin G is expressed by the phenotypically primitive mast cells within DD although its expression is minimal. We infer that cathepsin B and cathepsin D, and potentially cathepsin G, may provide bypass loops for the RAS expressed by the ESC-like population.

Although beyond the scope of this report, it is exciting to speculate on the possibility of targeting the ESC-like population within DD using RAS modulators, such as ACE inhibitors as previously proposed43 and inhibitors of cathepsins, such as curcumin44 for cathepsin B, pepstatin for cathepsin D,45 and chymostatin45 for cathepsin G, in the treatment of this condition.

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ACKNOWLEDGMENTS

The authors thank Ms. Liz Jones and Ms. Alice Chibnall of the Gillies McIndoe Research Institute for their assistance in IHC staining and performing tissue processing for NanoString analysis, respectively.

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