Search tips
Search criteria 


Logo of plosonePLoS OneView this ArticleSubmit to PLoSGet E-mail AlertsContact UsPublic Library of Science (PLoS)
PLoS One. 2010; 5(11): e13973.
Published online 2010 November 15. doi:  10.1371/journal.pone.0013973
PMCID: PMC2981574

Cystatin C Deficiency Promotes Epidermal Dysplasia in K14-HPV16 Transgenic Mice

Niels Olsen Saraiva Câmara, Editor



Cysteine protease cathepsins are important in extracellular matrix protein degradation, cell apoptosis, and angiogenesis. Mice lacking cathepsins are protected from tumor progression in several animal models, suggesting that the regulation of cathepsin activities controls the growth of various malignant tumors.

Methods and Results

We tested the role of cathepsins using a mouse model of multistage epithelial carcinogenesis, in which the human keratin-14 promoter/enhancer drove the expression of human papillomavirus type 16 (HPV16) early region E6/E7 transgenes. During the progression of premalignant dysplasia, we observed increased expression of cysteine protease cathepsin S, but concomitantly reduced expression of cathepsin endogenous inhibitor cystatin C in the skin tissue extract. Absence of cystatin C in these transgenic mice resulted in more progression of dysplasia to carcinoma in situ on the face, ear, chest, and tail. Chest and ear skin extract real time PCR and immunoblot analysis, mouse serum sample ELISA, tissue immunohistological analysis, and tissue extract-mediated in vitro elastinolysis and collagenolysis assays demonstrated that cystatin C deficiency significantly increased cathepsin expression and activity. In skin from both the chest and ear, we found that the absence of cystatin C reduced epithelial cell apoptosis but increased proliferation. From the same tissue preparations, we detected significantly higher levels of pro-angiogenic laminin 5-derived γ2 peptides and concurrently increased neovascularization in cystatin C-deficient mice, compared to those from wild-type control mice.


Enhanced cathepsin expression and activity in cystatin C-deficient mice contributed to the progression of dysplasia by altering premalignant tissue epithelial proliferation, apoptosis, and neovascularization.


Cysteine protease cathepsins are secretory lysosomal proteases that mediate both intracellular and extracellular protein degradation. Besides degrading endocytosed unwanted proteins, cathepsins are critical in degrading extracellular matrix collagen, laminin, fibronectin, and elastin, thus playing essential roles in tumor growth [1], [2]. Secreted and cell membrane–bound forms of tumor cathepsins may relate to local cellular behavior in certain cancers [3], [4]. Studies have described increases in cathepsin levels for most invasive cancer types [5]. In cancers, the best-studied cathepsins include cathepsins B (CatB), L (CatL), and S (CatS). In an immunohistological study using samples from human colon cancer patients, CatB was overexpressed and correlated strongly with angiogenesis and regional lymph node metastasis [6]. CatB inhibition in glioblastoma cells via RNA interference (RNAi) resulted in impaired invasion, reduced cell–cell interaction with endothelial cells (EC), disruption of capillary network formation in vitro and in vivo, and inhibition of established glioma tumor growth and invasion in intracranial tumors in vivo [7], [8]. RNAi-mediated CatB inhibition also reduced meningioma cell migration and invasion and led to significant regression of pre-established orthotopic tumors [9]. In an ischemic hindlimb model, CatL-deficient mice showed reduced neovascularization. CatL-deficient EC were less able to support the vascularization at the site of ischemia than were wild-type EC [10]. Transfection of an anti-CatL single-chain variable fragment in human melanoma cells inhibited the tumorigenic and metastatic properties completely, therefore producing less angiogenic and smaller tumors [11]. Similar observations were made in a RIP-Tag2 transgenic mouse pancreatic islet cell carcinoma model, in which the rat insulin II promoter (RIP) drove expression of the SV40 large T-antigen (Tag). These tumors also had increased cathepsin expression, which associated with angiogenic vasculature along the invasive front. Reduction in the activity of cathepsins using the pharmacologic inhibitor JPM, or deficiency of CatS, impaired angiogenic switch in progenitor lesions, affecting angiogenesis, tumor growth, vascularity, and invasiveness [12], [13].

Cystatins are endogenous inhibitors of cysteinyl cathepsins. Cathepsin to cystatin ratio increases in most tumor types, compared to normal tissue, particularly for advanced cancers [14][17]. Cystatin C, the most important, abundant, and widely expressed cathepsin inhibitor in humans and animals, decreased with concomitant increase of CatB in high-grade gliomas [15]. Benign ovarian cancers had significantly higher cystatin C levels than did malignant tumors [17]; in prostate cancers, cystatin C levels also decreased at late stages [18]. Nearly 50% of cancers show decreased expression of cystatin C, and perhaps of other cystatins [19]. However, tumor cystatin levels vary widely. In prostate cancers, cystatin C levels remained high at early stages [18]. During colorectal cancer progression, cystatin C remained unchanged between stages, whereas CatB levels remained high at any stage [20]. Serum cystatin C levels are significantly higher in patients with ovarian cancers than in benign ovarian tumors or in healthy women, though serum CatB levels are not different [21]. Similar findings are observed in patients with head and neck squamous-cell carcinoma; serum cystatin C levels in these patients are higher than those from control groups [22]. These observations suggest that the relative ratio of cystatin C to cathepsins in tumor tissues in situ, and not solely the proteases or inhibitors or those in the circulation, are essential in regulating tumor growth.

One approach to directly evaluate the effect of cystatin C on tumor initiation and evolution uses animal models with either increased or decreased expression of this inhibitor. More than 10 years have passed since the generation of the first cystatin C–deficient mouse to test its function in cancers. When melanoma cells were injected intravenously, cystatin C–deficient lungs showed reduced metastasis, but subcutaneous growth of melanoma cells was not different from that in control mice [23]. In contrast, cystatin C overexpression was associated with decreased glioblastoma cell invasion in vitro and tumor growth in vivo [24]. Such overexpression caused higher apoptosis in vivo for metastatic melanoma cells [25], and dramatically blocked lung metastasis of human fibrosarcoma cells (~90%) in mice [26]. To date, however, there has been no rigorous experimental examination of how this cathepsin inhibitor participates in tumor growth.

In this study, we introduced cystatin C mutant alleles into the invasive epidermis multistage squamous-cell carcinoma (SCC) mouse model [27], in which the human keratin-14 promoter/enhancer drove the expression of human papillomavirus HPV16 early region genes, including the E6/E7 oncogenes, to test whether absence of this dominant cathepsin inhibitor alters the progression of premalignant dysplasia. This established dysplasia to carcinoma model [27] is characterized by temporally and histopathologically reproducible, multi-stage progression of dysplasia by 3 months to SCC by 9 months. Accordingly, it is ideal for evaluation of the effect of cystatin C on cancer progression via the gene knockout approach.

Materials and Methods

Mice and ethics

Cystatin C–deficient (Cstc−/−) mice (C57BL/6/S129 background) [23] were backcrossed to an FVB/n background (Jackson Laboratories, Bar Harbor, ME) for >5 generations. These mice were crossbred with K14-HPV16 transgenic mice [27] (kindly provided by Dr. Lisa Coussen from the University of California, San Francisco), in the same FVB/n genetic background to ensure early-stage (at 3 months) dysplasia. K14-HPV16 transgenic Cstc−/− and Cstc+/+ wild-type littermates were sacrificed at 3 months of age. Chest and ear skin were collected and immediately embedded in compound OCT (optimum cutting temperature) for frozen section preparation (6 µm) or pulverized in liquid nitrogen to prepare tissue extracts for protein (lysed in a pH 5.5 buffer containing 1% Triton X-100, 40 mM sodium acetate, and 1 mM EDTA) or total RNA (lysed in TRIzol reagent; Stratagene, La Jolla, CA) preparation.

To test CatS and cystatin C expression during the progression of hyperplasia and dysplasia, we harvested skin tissues from K14-HPV16 transgenic mice at 1 month, 3 months, and 6 months of age for immunoblot analysis. Due to severe skin premalignant dysplasia from the K14-HPV16 transgenic Cstc−/− mice after 3 months of age, we were unable to study mice beyond this time point, for compliance with the humane standard of the Animal Research Committee of Harvard Medical School (approved animal protocol number 03759).

Real-time PCR

Real-time polymerase chain reaction (RT-PCR) was used to determine cathepsin transcript levels, including CatK, CatL, CatS, and CatB, in both chest skin and ear skin from 3-month-old K14-HPV16 transgenic Cstc+/+ and Cstc−/− mice. Total cellular RNA was extracted from TRIzol reagent-treated tumor tissue extracts. RNase-free DNase (Ambion, Austin, TX) was used to remove genomic DNA contaminants. Equal amounts of RNA were reverse-transcribed, and quantitative PCR was assessed in a single-color RT-PCR detection system (Stratagene). The level of each cathepsin transcript was normalized to that of the β-actin transcript.

Western blot

Protein concentration of each tumor extract in pH 5.5 buffer was determined using Bio-Rad DC protein assay kit (Bio-Rad, Hercules, CA). An equal amount of protein (30 µg/sample) of each tissue extract preparation was separated on 14% SDS-PAGE, followed by immunoblot analysis with rabbit anti-human cathepsins S, L, and K polyclonal antibodies (1[ratio]1000, Calbiochem, San Diego, CA) or rabbit anti-human cystatin C polyclonal antibodies (1[ratio]1000; DAKO Corp., Carpinteria, CA), all of which cross-reacted with mouse gene products. Goat anti-mouse β-actin polyclonal antibodies (1[ratio]5000, Santa Cruz Biotechnology, CA) were used to determine equal protein loading. Densitometry analysis (ImageJ software, Bethesda, MD) was used to determine the relative cathepsin protein levels in skin and ear tissues from K14-HPV16 transgenic Cstc+/+ and Cstc−/− mice.


To determine systemic cathepsin levels, mouse serum samples from Cstc+/+ and Cstc−/− mice were used directly for ELISA. ELISA for CatS, matrix metalloproteinase-9 (MMP-9) (R&D Systems, Inc., Minneapolis, MN), and CatL (Bender MedSystems Inc., Burlingame, CA) were used according to the manufacturers' protocols.

Collagenase and elastase activity assay

A total of 20 µg of chest and ear skin extract from K14-HPV16 transgenic Cstc+/+ and Cstc−/− mice was combined to a final volume of 100 µl in EDTA-containing pH 5.5 buffer that was optimized for measuring cysteinyl cathepsin activities, but not MMPs or other neutral serine proteases. Fluorogenic elastin (10 µg/well, DQ elastin, Invitrogen, Carlsbad, CA) or type I collagen (10 µg/well, Calbiochem) were added to a 96-well plate. After adding 3 mM of dithiothreitol (Sigma, St. Louis, MO), the plate was incubated at 37°C for 3 days and read at an excitation of 505 nm and emission of 515 nm. Data were presented as relative fluorescent units.


Frozen sections (6 µm) prepared from chest and ear skin of the K14-HPV16 transgenic Cstc+/+ and Cstc−/− mice were used for conventional histological (hematoxylin and eosin stain) and immunohistological analysis with rabbit anti-human CatS polyclonal antibody (1[ratio]170, cross-reacts with mouse CatS) [28]; rabbit anti-human Ki67 polyclonal antibody (1[ratio]750, NovoCastra Laboratories Ltd, Newcastle, UK); rat anti-mouse CD31 (1[ratio]150), Mac-3 (1[ratio]900), CD4 (1[ratio]90), and CD8 (1[ratio]100) monoclonal antibodies (Pharmingen, San Diego, CA); rabbit anti-mouse laminin 5 fragment γ2 polyclonal antibody (1[ratio]250) [29]; and the TUNEL staining kit (ApopTag® Plus Peroxidase In Situ Apoptosis Kit, Millipore, Billerica, MA). Immunostaining was analyzed using computer-assisted image analysis software (Image-Pro Plus; Media Cybernetics, Bethesda, MD). Data were presented as antigen-positive area (%) or cell number per mm2.

Statistical analysis

Due to our relatively small sample sizes and abnormal data point distribution, we used the non-parametric Mann-Whitney U test to examine the statistical significance for all data in this study. All data were presented as mean ± SEM. P<0.05 was considered statistically significant.


Cystatin C and CatS expression in early hyperplasia and dysplasia stages from K14-HPV16 transgenic mice

As discussed, expression of cathepsins and their inhibitors varies at different stages of tumor growth [22]. To examine whether CatS and cystatin C were also expressed differently during the progression of premalignant dysplasia, we collected chest skin tumor tissues at different stages from K14-HPV16 transgenic mice that were wild-type for cystatin C, including those tumors established at early (3 months) and late (6 months) stages of dysplasia. Immunoblot analysis demonstrated that CatS protein levels plateaued at 3~6 months of age. Normal skins or those from the early stage (e.g., 1 month) had negligible CatS proteins (Figure 1A). In contrast, normal skins had high levels of cystatin C protein, which then decreased during premalignant progression, although cystatin C protein did not completely disappear at the 3-month and 6-month progression stages (Figure 1B).

Figure 1
Immunoblot analysis for CatS and cystatin C in mouse chest skin tissue extracts.

Cystatin C deficiency enhanced SCC in K14-HPV16 transgenic mice

To test the effect of cystatin C in SCC, we introduced the K14-HPV16 transgene into Cstc−/− and Cstc+/+ littermate control mice by crossbreeding Cstc−/− mice [23] with K14-HPV16 transgenic mice [27]. Genomic DNA PCR confirmed the cystatin C genotypes in K14-HPV16 transgenic mice (data not shown). Due to the extent of malignant dysplasia in Cstc−/− K14-HPV16 transgenic mice at later time points (after 3 months), for humane purposes, we sacrificed the K14-HPV16 transgenic mice that were Cstc+/+and Cstc−/− at 3 months of age for the remainder of the study. Anti-human cystatin C polyclonal antibody–mediated immunoblot analysis of chest skin tissue extracts from 3-month-old Cstc−/− and Cstc+/+ K14-HPV16 transgenic mice confirmed the absence of cystatin C in Cstc−/− mice (Figure 1C). At the 3-month time point, we observed SCC formation that was clinically more pronounced in skin from the chest (Figure 2A), tail (Figure 2B/C), face, and ear (Figure 2D/E) from the Cstc−/− mice as compared with that of the Cstc+/+ mice. These differences were confirmed histologically (Figure 2F–I); whereas back and ear skin from Cstc+/+ mice exhibited dysplasia (nuclear atypia and disordered maturation in epidermal cells, primarily within the lowermost layers), abnormalities were present uniformly throughout a thickened and more hyperkeratotic epidermal layer in the Cstc−/− mice, thus qualifying for a designation of SCC in situ. Such SCC formation or dysplasia was absent in Cstc−/− or Cstc+/+ mice without the K14-HPV16 transgene (not shown). Therefore, absence of cystatin C enhanced dysplasia to SCC progression in site-matched skin in the K14-HPV16 transgenic mice.

Figure 2
Enhanced epidermal dysplasia in cystatin C-deficient K14-HPV16 transgenic mice.

Cystatin C deficiency increased cysteinyl cathepsin expression and activities

Enhanced SCC formation in Cstc−/− K14-HPV16 transgenic mice compared with those wild-type for cystatin C suggests the importance of this endogenous cathepsin inhibitor in early tumor progression in vivo. The development of SCC in Cstc−/− K14-HPV16 transgenic mice possibly results from altered counterbalance between cystatin C and cathepsins. To test this hypothesis, we prepared total RNA from chest and ear skin and performed RT-PCR. Absence of cystatin C significantly increased the RNA levels of cathepsins L, S, and B in the chest skin and of CatL in the ear skin (Figure 3A/B). Tumor tissue extract immunoblot analysis using protein samples from the chest skin (Figure 3C) or the ear skin (Figure 3D) also revealed significantly increased CatS protein in the chest skin extracts (Figure 3E) and CatK and CatL proteins in the ear skin extracts (Figure 3F), as determined by densitometric measurements. In serum from K14-HPV16 transgenic Cstc+/+ and Cstc−/− mice, we made similar observations. Serum from the Cstc−/− mice had significantly higher levels of both CatS (Figure 4A) and CatL (Figure 4B) than that from the Cstc+/+ mice, whereas cystatin C deficiency did not significantly affect serum MMP-9 levels (Figure 4C). Chest and ear skin immunohistological analysis also revealed increased expression of CatS throughout the epidermis and dermis from Cstc−/− mice, compared with those from Cstc+/+ mice (Figure 5).

Figure 3
Cystatin C deficiency affects cathepsin expression and activity.
Figure 4
Serum protease levels.
Figure 5
Immunostaining for CatS in chest and ear skin tumor sections.

Absence of cystatin C also enhanced tumor tissue extract cathepsin activities. Upon incubating chest and ear skin extracts in pH 5.5 buffer, which measures only cysteinyl cathepsins [30], with fluorogenic elastin and collagen, two common matrix protein substrates for cathepsins S, L, K, and B, we found that tumor tissue extracts from both the chest skin and ear skin from Cstc−/− mice had significantly higher elastase (Figure 6A) and collagenase (Figure 6B) activities than those from Cstc+/+ mice. Together, our data demonstrated increased expression and activities of cysteinyl cathepsins in the absence of cystatin C.

Figure 6
Mouse chest and ear skin tissue extract elastase and collagenase assays.

Tumor progression often accompanies inflammatory cell infiltrations [31][33], including monocytes/macrophages, B and T lymphocytes, NK cells, and neutrophils. These infiltrates often influence the tumor progression directly. For example, in the same K14-HPV16 transgenic mice used in this study, deficiency of CD4+ T cells delays neoplastic progression and lowers tumor incidence [33]. These cells are rich in cathepsin expression and activities [34], [35]. Therefore, increased cysteinyl cathepsin expression and activities in SCC chest and ear skin tissues from Cstc−/− mice can be the results of the absence of cystatin C as well as of enhanced inflammatory cell infiltration. To examine this hypothesis, we immunostained both the chest and ear sections from Cstc+/+ and Cstc−/− mice for CD4, CD8, and macrophage marker Mac-3. Both chest and ear sections from Cstc−/− mice contained significantly higher percentages of CD4-positive areas than did the Cstc+/+ mice (Figure 7A). Mac-3–positive areas were also higher in the ear sections, but not in the chest sections, from Cstc−/− mice than from Cstc+/+ mice (Figure 7B). There were no differences, however, in CD8-positive areas in chest sections (10.53±4.35 vs. 8.40±3.44, P = 0.252) and ear sections (6.37±3.79 vs. 7.34±0.56, P = 0.096) between Cstc−/− and Cstc+/+ mice. Increased infiltration of CD4+ T cells and Mac-3+ macrophages in Cstc−/− mice may account in part for enhanced lesion cathepsin activities in chest and ear skin from these mice (Figures 3C–3F, ,5,5, and and66).

Figure 7
Immunostaining for inflammatory cells in chest and ear skin tumor sections.

Decreased apoptosis and increased cell proliferation in cystatin C–deficient SCC

Tumor cell apoptosis and proliferation are major determinants of growth or progression of cancers [36], [37]. The development of fully evolved in situ SCC in Cstc−/− mice, but not in Cstc+/+ mice, suggests that cystatin C deficiency may reduce tumor cell apoptosis and/or increase tumor cell proliferation. To test this possibility, we immunostained both the chest and ear skin tissue frozen sections for TUNEL and for the cell proliferation marker Ki67. Consistent with our hypothesis, tumor tissues (chest and ear skin) from Cstc−/− mice had significantly fewer total apoptotic cells than those from Cstc+/+ mice (Figure 8A). In Cstc+/+ mouse chest skin, most apoptotic cells were noted in the epidermis and hair sebaceous unit areas. Relatively fewer apoptotic cells appeared in the dermis. However, in Cstc−/− mouse chest skin, both the epidermis and sebaceous unit showed noteworthy reduction of apoptotic cells. In contrast, apoptotic cells from the Cstc+/+ mouse ear skin clustered in the dermis, while ear skin from the Cstc−/− mice had significantly reduced levels of such apoptotic cells (Figure 8A). Significantly more Ki67-positive proliferating cells were identified in the epidermis and sebaceous units from chest skin of the Cstc−/− mice than in those from the Cstc+/+ mice (Figure 8B). Reduced apoptosis, but increased proliferation in the epidermis and sebaceous unit of Cstc−/− mice, thus correlates with progression to SCC in situ. Similar findings were documented in the Cstc−/− mouse ear skin. In the epidermis of Cstc−/− mouse ear skin, we detected significantly more Ki67-positive cells than in that of the Cstc+/+ mice (Figure 8B). In summary, cystatin C deficiency increased cell proliferation but decreased cell apoptosis, thus correlating with progression to SCC in situ in both chest and ear skin, events that likely also developed at other similarly affected sites (e.g., tail and face skin; Figure 2).

Figure 8
Immunostaining for apoptotic and proliferating cells in chest and ear skin tumor sections.

Cystatin C deficiency led to increased angiogenesis

Cysteinyl cathepsin-mediated angiogenesis is important in cancer progression and tumor growth. We reported that in the pancreatic islet cell carcinoma RIP-Tag2 model, absence of CatS significantly reduced tumor growth [13]. Mechanistically, we demonstrated that CatS mediates extracellular matrix laminin-5 degradation, followed by the production of a pro-angiogenic peptide from laminin-5 proteolysis, named γ2 [13], [29]. In CatS-deficient mice, along with reduced tumor growth, we detected significant reduction of this γ2 fragment, and concomitantly, greatly impaired angiogenesis [13]. Along with producing the γ2 fragment from laminin-5, cysteinyl cathepsins mediate other matrix protein degradation, all of which relate to angiogenesis and tumor growth. In the present study, we conjectured that the absence of cystatin C caused increased cathepsin expression and activities (Figures 36)6) and enhanced pro-angiogenic γ2 production with promotion of angiogenesis, leading to increased progression to SCC (Figure 2). To test this hypothesis, we performed immunohistological analysis of both chest and ear skin from the Cstc+/+ and Cstc−/− mice. Consistent with our hypothesis, we detected significantly more γ2-positive microvessels in the dermis of both chest and ear skin of Cstc−/− mice than in those of Cstc+/+ mice (Figure 9A). Along with increased γ2 production in Cstc−/− mouse chest and ear skin, we observed significant enhancement of CD31-positive microvessels in the skin of these mice, more than twice as many as those from Cstc+/+ mice (Figure 9B). Increased angiogenesis in Cstc−/− mouse skin may relate to associated progression to SCC.

Figure 9
Immunostaining for microvessels in chest and ear skin tumor sections.


Protease and protease inhibitor counterbalance prove physiologically important and pathologically relevant in human diseases. Increased protease activities, either by increased protease expression or decreased protease inhibitor expression, lead to many common human disorders, such as cardiovascular diseases, metabolic conditions, bone metabolic dysfunction, cancers, and neurological complications. We have previously shown that the absence of cystatin C enhanced atherogenesis in apolipoprotein E-deficient (Apoe−/−) mice [38]. One mechanism of advanced atherogenesis in these Apoe−/− mice, increased cathepsin activities, leads to enhanced elastinolysis and collagenolysis, and thus to blood-borne leukocyte accumulation in the neointima. In the present study, although using a different disease model, we found that cystatin C deficiency results in enhanced SCC progression involving a similar mechanism to what we have observed in the cardiovascular system. Absence of this cathepsin inhibitor enhanced cathepsin expression and activity, which altered epidermal cell kinetics and advanced angiogenesis, thereby expediting cancer progression.

The function of cathepsins in angiogenesis has been well studied in several disease models [39]. In general, angiogenesis involves extensive extracellular matrix protein degradation and tissue remodeling, which requires protease involvement. But cathepsins can achieve more than just matrix protein degradation. In vitro studies showed that CatB and CatL can liberate collagen IV, laminin, and fibronectin from the basement membrane, generate gelatinolytic fragments, and initiate a “metastatic cascade,” thereby promoting angiogenesis and tumor invasion [40]. We recently have shown that CatS degrades the anti-angiogenic peptides arresten, canstatin, and tumstatin, all of which constitute collagen IV degradation products [13], [41]. Further, CatS degrades the natural basement membrane matrix protein laminin-5, and generates pro-angiogenic γ2 fragments in vitro [13], [29]. Cysteinyl cathepsin proteolysis of these latent matrix proteins therefore is critical in regulating angiogenesis, and thus in tumor invasion, as we found in the CatS-deficient RIP-Tag2 model. Absence of CatS reduced γ2 fragment production, and consequently reduced islet-cell carcinoma growth [13]. In the present study, we also detected significantly higher amounts of CatS (Figure 5) and CatS-derived laminin-5 γ2 fragments (Figure 9A) in chest and ear skin lesions from Cstc−/− mice than in those from Cstc+/+ mice. These observations furnish a mechanistic explanation of the increased angiogenesis detected from the chest and ear skin of the Cstc−/− mice, compared with those from the Cstc+/+ mice (Figure 9B).

Cancer cell proliferation and apoptosis closely relate to angiogenesis, and therefore are important in tumor growth. Angiogenesis provides cancer cells with sufficient nutrients for survival and proliferation; reduced angiogenesis thus may cause cancer cell apoptosis or decreased cell proliferation. In return, cancer-cell apoptosis and proliferation can also regulate angiogenesis. Cysteinyl cathepsins can participate importantly in these processes. When co-cultured with human glioblastoma cells, human microvascular EC increased the invasiveness of the glioblastoma cells. On the other hand, glioblastoma cells stimulated microvascular EC proliferation, which CatB-selective inhibitor CA074me can impair [42]. Therefore, increased expression of CatB may enhance EC proliferation in vivo. Although we saw increased expression of several important cathepsins and enhanced cancer cell proliferation in chest and ear skin sections from Cstc−/− mice (Figure 8B), whether the increase of proliferation associated with angiogenesis remains unknown. Our observation of reduced cancer-cell apoptosis in chest and ear skin from Cstc−/− mice (Figure 8A) gives some support to this hypothesis.

Although we anticipated enhanced angiogenesis and tumor growth in Cstc−/− mice, several aspects of our results remain unexplained, and more studies are required for further understanding of the role of cathepsins in tumorigenesis. First, we frequently have seen that absence of one protease affects the expression of the others — for example, vascular cells from serine protease chymase-deficient [43] or tryptase-deficient (unpublished data) mice express significantly reduced levels of cathepsins. We demonstrated in this study that deficiency of cystatin C increased both RNA and protein levels of most, if not all, tested cathepsins. Second, cathepsins are thought to promote cell apoptosis — for example, CatB cleaves the anti-apoptotic protein Bcl-2 member Bid and creates a pro-apoptotic signal of mitochondrial cytochrome C release [44]. Osteosarcoma cell line U2OS, overexpressing HPV oncogene E7 and cell cycle regression regulator p21, undergoes apoptosis in a CatB-dependent but caspase-independent manner. CatB-selective inhibitor CA074me significantly blocked U2OS cell death [45]. Thus, CatB-deficient mice showed reduced cerebral cell losses, whereas a cystatin mutation resulted in increased apoptosis of cerebellar granule cells [46]. A direct role for cathepsins in promoting apoptosis does not explain our finding in this study of increased cathepsin expression and activities, but reduced cancer apoptosis (Figures 36,6, Figure 8A). One possibility is that increased cathepsin expression and activities in Cstc−/− mice enhanced extracellular matrix processing, which may explain why we detected more laminin-5 fragment γ2 (Figure 9A) and increased angiogenesis (Figure 9B). Compared with the chest and ear skin from Cstc−/− mice, we found significantly lower numbers of microvessels in the Cstc+/+ mice (Figure 9B). Reduced angiogenesis in Cstc+/+ mice may affect nutrient supply, thus increasing cell death and reducing proliferation, although a detailed mechanism of cathepsin function in this SCC cancer model requires further investigation. Third, it is conceivable that angiogenesis is essential for tumorigenesis after angiogenic switch, but less so in early stages. Our data demonstrated that enhanced cathepsin expression expedited malignant transformation, which also can be caused by alterations in growth factor levels, inflammatory cell infiltration (Figure 7), and associated intracellular signaling. Mechanisms in addition to enhanced angiogenesis may account for more advanced tumorigenesis in Cstc−/− mice than in Cstc+/+ mice.

In conclusion, this study provides additional in vivo evidence to support direct participation of cysteinyl cathepsins in tumor growth. Based on these findings, we conjecture that the absence of cystatin C also may increase the progression and growth of other types of tumors. Thus, inhibition of cysteinyl cathepsins, either by small molecular inhibitors [47], antibody therapy [48], or retrovirus-mediated cathepsin inhibitor delivery [49], holds potential for the development of novel cancer therapies.


The authors thank Dr. Lisa Coussen from the Department of Pathology, University of California, San Francisco, for providing the K14-HPV16 transgenic mice. The authors also thank Mrs. Eugenia Shvartz for technical assistance, and Ms. Sara Karwacki for editorial assistance.


Competing Interests: The authors have declared that no competing interests exist.

Funding: This study is supported by National Institutes of Health grants HL60942, HL81090, HL88547 (GPS); HL56985 (PL); and Established Investigator Award (0840118N) from the American Heart Association (GPS). The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.


1. Szpaderska AM, Frankfater A. An intracellular form of cathepsin B contributes to invasiveness in cancer. Cancer Res. 2001;61:3493–3500. [PubMed]
2. Premzl A, Zavasnik-Bergant V, Turk V, Kos J. Intracellular and extracellular cathepsin B facilitate invasion of MCF-10A neoT cells through reconstituted extracellular matrix in vitro. Exp Cell Res. 2003;283:206–214. [PubMed]
3. Moin K, Cao L, Day NA, Koblinski JE, Sloane BF. Tumor cell membrane cathepsin B. Biol Chem. 1998;379:1093–1099. [PubMed]
4. Erdel M, Trefz G, Spiess E, Habermaas S, Spring H, et al. Localization of cathepsin B in two human lung cancer cell lines. J Histochem Cytochem. 1990;38:1313–1321. [PubMed]
5. Mohamed MM, Sloane BF. Cysteine cathepsins: multifunctional enzymes in cancer. Nat Rev Cancer. 2006;6:764–775. [PubMed]
6. Kruszewski WJ, Rzepko R, Wojtacki J, Skokowski J, Kopacz A, et al. Overexpression of cathepsin B correlates with angiogenesis in colon adenocarcinoma. Neoplasma. 2004;51:38–43. [PubMed]
7. Lakka SS, Gondi CS, Yanamandra N, Olivero WC, Dinh DH, et al. Inhibition of cathepsin B and MMP-9 gene expression in glioblastoma cell line via RNA interference reduces tumor cell invasion, tumor growth and angiogenesis. Oncogene. 2004;23:4681–4689. [PubMed]
8. Yanamandra N, Gumidyala KV, Waldron KG, Gujrati M, Olivero WC, et al. Blockade of cathepsin B expression in human glioblastoma cells is associated with suppression of angiogenesis. Oncogene. 2004;23:2224–2230. [PubMed]
9. Tummalapalli P, Spomar D, Gondi CS, Olivero WC, Gujrati M, et al. RNAi-mediated abrogation of cathepsin B and MMP-9 gene expression in a malignant meningioma cell line leads to decreased tumor growth, invasion and angiogenesis. Int J Oncol. 2007;31:1039–1050. [PMC free article] [PubMed]
10. Urbich C, Heeschen C, Aicher A, Sasaki K, Bruhl T, et al. Cathepsin L is required for endothelial progenitor cell-induced neovascularization. Nat Med. 2005;11:206–213. [PubMed]
11. Rousselet N, Mills L, Jean D, Tellez C, Bar-Eli M, et al. Inhibition of tumorigenicity and metastasis of human melanoma cells by anti-cathepsin L single chain variable fragment. Cancer Res. 2004;64:146–151. [PubMed]
12. Joyce JA, Baruch A, Chehade K, Meyer-Morse N, Giraudo E, et al. Cathepsin cysteine proteases are effectors of invasive growth and angiogenesis during multistage tumorigenesis. Cancer Cell. 2004;5:443–453. [PubMed]
13. Wang B, Sun J, Kitamoto S, Yang M, Grubb A, et al. Cathepsin S controls angiogenesis and tumor growth via matrix-derived angiogenic factors. J Biol Chem. 2006;281:6020–6029. [PubMed]
14. Yoshii A, Kageshita T, Tsushima H, Ono T. Clinical relevance of cathepsin B-like enzyme activity and cysteine proteinase inhibitor in melanocytic tumours. Arch Dermatol Res. 1995;287:209–213. [PubMed]
15. Nakabayashi H, Hara M, Shimuzu K. Clinicopathologic significance of cystatin C expression in gliomas. Hum Pathol. 2005;36:1008–1015. [PubMed]
16. Krepela E, Procházka J, Kárová B, Cermák J, Roubková H. Cysteine proteases and cysteine protease inhibitors in non-small cell lung cancer. Neoplasma. 1998;45:318–331. [PubMed]
17. Nishikawa H, Ozaki Y, Nakanishi T, Blomgren K, Tada T, et al. The role of cathepsin B and cystatin C in the mechanisms of invasion by ovarian cancer. Gynecol Oncol. 2004;92:881–886. [PubMed]
18. Jiborn T, Abrahamson M, Gadaleanu V, Lundwall A, Bjartell A. Aberrant expression of cystatin C in prostate cancer is associated with neuroendocrine differentiation. BJU Int. 2006;98:189–196. [PubMed]
19. Sokol JP, Schiemann WP. Cystatin C antagonizes transforming growth factor beta signaling in normal and cancer cells. Mol Cancer Res. 2004;2:183–195. [PubMed]
20. Hirai K, Yokoyama M, Asano G, Tanaka S. Expression of cathepsin B and cystatin C in human colorectal cancer. Hum Pathol. 1999;30:680–686. [PubMed]
21. Nishikawa H, Ozaki Y, Nakanishi T, Blomgren K, Tada T, et al. The role of cathepsin B and cystatin C in the mechanisms of invasion by ovarian cancer. Gynecol Oncol. 2004;92:881–886. [PubMed]
22. Strojan P, Svetic B, Smid L, Kos J. Serum cystatin C in patients with head and neck carcinoma. Clin Chim Acta. 2004;344:155–161. [PubMed]
23. Huh CG, Håkansson K, Nathanson CM, Thorgeirsson UP, Jonsson N, et al. Decreased metastatic spread in mice homozygous for a null allele of the cystatin C protease inhibitor gene. Mol Pathol. 1999;52:332–340. [PMC free article] [PubMed]
24. Konduri SD, Yanamandra N, Siddique K, Joseph A, Dinh DH, et al. Modulation of cystatin C expression impairs the invasive and tumorigenic potential of human glioblastoma cells. Oncogene. 2002;21:8705–8712. [PubMed]
25. Ervin H, Cox JL. Late stage inhibition of hematogenous melanoma metastasis by cystatin C over-expression. Cancer Cell Int. 2005;5:14. [PMC free article] [PubMed]
26. Kopitz C, Anton M, Gansbacher B, Krüger A. Reduction of experimental human fibrosarcoma lung metastasis in mice by adenovirus-mediated cystatin C overexpression in the host. Cancer Res. 2005;65:8608–8612. [PubMed]
27. Coussens LM, Hanahan D, Arbeit JM. Genetic predisposition and parameters of malignant progression in K14-HPV16 transgenic mice. Am J Pathol. 1996;149:1899–1917. [PubMed]
28. Shi GP, Webb AC, Foster KE, Knoll JH, Lemere CA, et al. Human cathepsin S: chromosomal localization, gene structure, and tissue distribution. J Biol Chem. 1994;269:11530–11536. [PubMed]
29. Sasaki T, Göhring W, Mann K, Brakebusch C, Yamada Y, et al. Short arm region of laminin-5 gamma2 chain: structure, mechanism of processing and binding to heparin and proteins. J Mol Biol. 2001;314:751–763. [PubMed]
30. Sukhova GK, Shi GP, Simon DI, Chapman HA, Libby P. Expression of the elastolytic cathepsins S and K in human atheroma and regulation of their production in smooth muscle cells. J Clin Invest. 1998;102:576–583. [PMC free article] [PubMed]
31. Ortegel JW, Staren ED, Faber LP, Warren WH, Braun DP. Cytokine biosynthesis by tumor-infiltrating T lymphocytes from human non-small-cell lung carcinoma. Cancer Immunol Immunother. 2000;48:627–634. [PubMed]
32. Neuchrist C, Grasl M, Scheiner O, Lassmann H, Ehrenberger K, et al. Squamous cell carcinoma: infiltrating monocyte/macrophage subpopulations express functional mature phenotype. Br J Cancer. 1990;62:748–753. [PMC free article] [PubMed]
33. Daniel D, Meyer-Morse N, Bergsland EK, Dehne K, Coussens LM, et al. Immune enhancement of skin carcinogenesis by CD4+ T cells. J Exp Med. 2003;197:1017–1028. [PMC free article] [PubMed]
34. Shi GP, Bryant RA, Riese R, Verhelst S, Driessen C, et al. Role for cathepsin F in invariant chain processing and major histocompatibility complex class II peptide loading by macrophages. J Exp Med. 2000;191:1177–1186. [PMC free article] [PubMed]
35. Kitamoto S, Sukhova GK, Sun J, Yang M, Libby P, et al. Cathepsin L deficiency reduces diet-induced atherosclerosis in low-density lipoprotein receptor-knockout mice. Circulation. 2007;115:2065–2075. [PubMed]
36. Evan GI, Vousden KH. Proliferation, cell cycle and apoptosis in cancer. Nature. 2001;411:342–348. [PubMed]
37. Klein S, McCormick F, Levitzki A. Killing time for cancer cells. Nat Rev Cancer. 2005;5:573–580. [PubMed]
38. Sukhova GK, Wang B, Libby P, Pan JH, Zhang Y, et al. Cystatin C deficiency increases elastic lamina degradation and aortic dilatation in apolipoprotein E-null mice. Circ Res. 2005;96:368–375. [PubMed]
39. Yasuda Y, Kaleta J, Brömme D. The role of cathepsins in osteoporosis and arthritis: rationale for the design of new therapeutics. Adv Drug Deliv Rev. 2005;57:973–993. [PubMed]
40. Guinec N, Dalet-Fumeron V, Pagano M. “In vitro” study of basement membrane degradation by the cysteine proteinases, cathepsins B, B-like and L Digestion of collagen IV, laminin, fibronectin, and release of gelatinase activities from basement membrane fibronectin. Biol Chem Hoppe Seyler. 1993;374:1135–1146. [PubMed]
41. Mundel TM, Kalluri R. Type IV collagen-derived angiogenesis inhibitors. Microvasc Res. 2007;74:85–89. [PubMed]
42. Kenig S, Alonso MB, Mueller MM, Lah TT. Glioblastoma and endothelial cells cross-talk, mediated by SDF-1, enhances tumour invasion and endothelial proliferation by increasing expression of cathepsins B, S, and MMP-9. Cancer Lett. 2010;289:53–61. [PubMed]
43. Sun J, Zhang J, Lindholt JS, Sukhova GK, Liu J, et al. Critical role of mast cell chymase in mouse abdominal aortic aneurysm formation. Circulation. 2009;120:973–982. [PMC free article] [PubMed]
44. Stoka V, Turk B, Schendel SL, Kim TH, Cirman T, et al. Lysosomal protease pathways to apoptosis. Cleavage of bid, not pro-caspases, is the most likely route. J Biol Chem. 2001;276:3149–3157. [PubMed]
45. Kaznelson DW, Bruun S, Monrad A, Gjerløv S, Birk J, et al. Simultaneous human papilloma virus type 16 E7 and cdk inhibitor p21 expression induces apoptosis and cathepsin B activation. Virology. 2004;320:301–312. [PubMed]
46. Pennacchio LA, Bouley DM, Higgins KM, Scott MP, Noebels JL, et al. Progressive ataxia, myoclonic epilepsy and cerebellar apoptosis in cystatin B-deficient mice. Nat Genet. 1998;20:251–258. [PubMed]
47. Gocheva V, Zeng W, Ke D, Klimstra D, Reinheckel T, et al. Distinct roles for cysteine cathepsin genes in multistage tumorigenesis. Genes Dev. 2006;20:543–556. [PubMed]
48. Burden RE, Gormley JA, Jaquin TJ, Small DM, Quinn DJ, et al. Antibody-mediated inhibition of cathepsin S blocks colorectal tumor invasion and angiogenesis. Clin Cancer Res. 2009;15:6042–6051. [PubMed]
49. Frade R, Rousselet N, Jean D. Intratumoral gene delivery of anti-cathepsin L single-chain variable fragment by lentiviral vector inhibits tumor progression induced by human melanoma cells. Cancer Gene Ther. 2008;15:591–604. [PubMed]

Articles from PLoS ONE are provided here courtesy of Public Library of Science