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Departments of 1Pathology and Laboratory Medicine, 2Internal Medicine, and 5Surgery, University Medical Center Groningen and University of Groningen, Groningen, The Netherlands; 3Renal Division, Brigham and Women's Hospital, Harvard Medical School, Boston; and 4Biogen, Incorporated, Cambridge, Massachusetts
Submitted 13 October 2005 ; accepted in final form 1 February 2006
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ABSTRACT |
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 TOP ABSTRACT MATERIALS AND METHODSRESULTSDISCUSSIONGRANTSREFERENCES |
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-actin, 4.08 ± 2.56 vs. 0.52 ± 0.64 in NX, P < 0.001) and localized to damaged tubules. Kim-1 protein expression was markedly induced in NX+BSA (2.46 ± 1.19 vs. 0.39 ± 0.10% staining/field in NX, P < 0.001). Urinary Kim-1 was significantly elevated in NX+BSA (921 ± 592 vs. 87 ± 164 pg/ml in NX, P < 0.001) and correlated with tissue Kim-1 expression (r = 0.66, P =0.02). Kim-1 protein was found at the apical membrane of dilated nephrons. Kim-1 expression was limited to areas with inflammation (MØ), fibrosis (
-smooth muscle actin), and tubular damage (osteopontin), and only occasionally with tubular dedifferentiation (vimentin). These results implicate involvement of Kim-1 in the pathogenesis of proteinuria-induced renal damage/repair. Urinary Kim-1 levels may serve as a marker of proteinuria-induced renal damage. tubulointerstitial damage; proximal tubular cell; proteinuria; renal pathology
Kidney injury molecule-1 (Kim-1) is a recently discovered tubular protein that is markedly induced after ischemia-reperfusion injury and in response to a number of other proximal tubular toxins, including cisplatin and folic acid (10, 11). Kim-1 is a type I transmembrane glycoprotein, with an ectodomain containing an Ig-like domain and a mucin domain. In normal kidneys, Kim-1 is undetectable, but this molecule is abundantly expressed in PTC after ischemic (10) and nephrotoxic injury (11). In mice, Kim-1 is upregulated in polycystic kidney disease especially in regions of the kidney where there is fibrosis (14). In humans and in rodents, Kim-1 is induced after ischemic or toxic acute tubular necrosis and the cleaved Kim-1 ectodomain is quantified in the urine as a biomarker for acute kidney injury (9, 21). This ectodomain shedding is confirmed in cultured human PTC where cleavage and shedding could be blocked by inhibition of metalloproteinase activity (1).
The early and abundant tubular expression following different types of injury makes Kim-1 a specific marker of tubular cell injury that may be linked to recuperative or damaging mechanisms that direct the process of interstitial damage, as has been proposed previously (14). Proteinuria has been proposed to cause tubular injury and interstitial fibrosis, therefore we studied Kim-1 expression in a nontoxic model of acute massive proteinuria, protein-overload nephropathy. In addition, we investigated whether urinary Kim-1 levels reflect renal tissue damage.
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MATERIALS AND METHODS |
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Protein-overload nephropathy was induced 1 wk after left nephrectomy in male Wistar rats (Harlan, Horst, The Netherlands), weighing 262 ± 13 g (means ± SD). Rats received intraperitoneal (ip) injections of 7 ml PBS (NX; n = 6) or 2 g BSA (low-endotoxin BSA, Sigma-Aldrich, Zwijndrecht, The Netherlands) dissolved in 7 ml PBS (NX+BSA; n = 12) six times a week for 3 consecutive weeks under isoflurane anesthesia. Rats were housed in a light- and temperature-controlled environment with free access to water and standard rat chow. Procedures were approved by the Committee for Animal Experiments of the University of Groningen, and the Principles of Laboratory Animal Care (NIH publication no. 85–23) were followed.
Body weight was measured weekly. Urine was collected weekly during a 24-h stay in metabolic cages with access to drinking water only. Tail vein blood samples were taken weekly under anesthesia. At the end of the study, rats were anesthetized, a blood sample was taken by cannulation of the aorta, and kidneys were perfused with saline. A coronal tissue slice was snap-frozen in isopentane and stored at –80°C. Another slice was fixed in 4% paraformaldehyde for paraffin embedding.
Measurements in Blood and Urine
Proteinuria was measured colorimetrically with the Pyrogallol-Red Molybdate method. Plasma and urine creatinine levels were determined by the Jaffé method (Merck Mega, Darmstadt, Germany). Plasma triglycerides, cholesterol, and glucose were determined by the GPO-PAP, CHOD-PAP, and glucose dehydrogenase (Gluc-DH) methods (Merck Mega), respectively.
Kim-1 protein in urine was measured by microsphere-based Luminex xMAP technology (20). This technique is an adaptation of the recently developed and validated sandwich ELISA assay (21). For measurements, 30 µl of 24-h urine were analyzed in duplicate.
RNA Extraction and RT-PCR
Total RNA was isolated from 10 slices of 10 µm frozen tissue with TRIzol. cDNA was synthesized from 2 µg RNA by oligo(dT) priming (1 h) using a Sensiscript Reverse Transcriptase kit (Qiagen/Westburg, Leusden, The Netherlands). PCR was performed as described (22) with gene-specific primer pairs for Kim-1 and -actin: Kim-1 F, 5'-ACT CCT GCA GAC TGG AAT GG-3'; Kim-1 R, 5'-CAA AGC TCA GAG AGC CCA TC-3', generating a 213-bp PCR product; -actin F, 5'-AAC ACC CCA GCC ATG TAC G-3'; -actin R, 5'-ATG TCA CGC ACG ATT TCC C-3', generating a 253-bp PCR product. Cycles consisted of 40 s at 94°C, 40 s at 56°C, and 60 s at 72°C. The final extension was 7 min at 72°C. Each RNA sample was verified for the absence of genomic DNA by performing RT-PCR reactions without addition of an RT enzyme. The number of cycles was selected to allow for amplification within the linear range (34 for Kim-1, 24 for -actin). Amplified products were analyzed by electrophoresis on 1.2% agarose gels and scanned on an Imagemaster VDS (Amersham Biosciences, Little Chalfont, UK) using LISCAP software. PCR product abundance was quantified using Imagemaster 1D prime v3.00 (Amersham, Roosendaal, The Netherlands) and normalized for a -actin signal from the same cDNA.
In Situ Hybridization
A 696-bp Kim-1 PCR product was formed with the primers Kim-1 F, 5'-AAC GCA GCG ATT GTG CAT CC-3' and Kim-1 R, 5'-GTC CAC TCA CCA TGG TAA CC-3' and subcloned into the pCRII-TOPO vector (Invitrogen, Carlsbad, CA). DIG-labeled RNA probes were made with a DIG RNA labeling Kit (Sp6/T7, Roche, Mannheim, Germany). Deparaffinized sections were air-dried for 10 min and treated with Triton X-100, followed by proteinase K (5 µg/ml in TBS, Roche) at 37°C for 20 min. After being washed with PBS, slides were incubated with 10 ng/100 µl DIG-labeled probe (SP6/antisense or T7/sense) in hybridization solution consisting of 100 µl 50x Denhardt's solution, 1 ml 20x SSC, 1 ml 50% dextran sulfate, 2.5 ml formamide, 200 µl (25 mg/ml) t-RNA, 49 µl 1 M DTT and 125 µl (10 mg/ml) salmon sperm DNA overnight at 55°C. After being washed, slides were treated with 2 U/ml RNase (Sigma-Aldrich, Steinheim, Germany) at 37°C for 30 min. Positive cells were visualized with anti-DIG-labeled alkaline phosphatase (Roche) for 1 h at 37°C in 0.1 M maleic acid buffer containing 0.15 M NaCl, 1% blocking buffer, and 2% normal sheep serum. Alkaline phosphatase reactivity was developed for 1 h at 37°C, followed by 24–48 h at 4°C, using NBT and BCIP (Roche) in 1 ml TBS containing 50 mM MgCl2 and 0.01 M levamisole.
Immunohistochemistry
Deparaffinized sections (4 µm) were subjected to heat-induced antigen retrieval by overnight incubation in 0.1 M Tris·HCl buffer (pH 9.0) at 80°C. Endogenous peroxidase was blocked for 30 min with 0.075% H2O2 in PBS. Primary antibodies (Table 1), diluted in 1% BSA/PBS, were incubated for 60 min at room temperature. Binding was detected using sequential incubations (30 min, Table 1) with appropriate peroxidase-labeled secondary antibodies (DakoCytomation) diluted in PBS with 1% BSA and 1% normal rat serum. Peroxidase activity was developed using 3,3'-diaminobenzidine tetrachloride (DAB) for 10 min. Sections were counterstained with periodic acid-Schiff (PAS) and hematoxylin. Appropriate isotype and PBS controls were consistently negative.
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-smooth muscle actin (-SMA; 50 glomeruli) and interstitial collagen III, osteopontin (OPN), -SMA, and Kim-1 (30 randomly selected cortical fields; vessels and glomeruli were excluded). The total staining area was divided by the total surface area and expressed as a percentage. For glomerular macrophages (MØ), the number of positive cells per glomerulus (n = 50) was counted. The number of interstitial MØ was counted in 30 interstitial fields. Glomerular desmin staining was semiquantitatively scored (0–4, 50 glomeruli) by estimating the percentage of desmin-positive visceral epithelial cells in the outer cell layer of the glomerular tuft. A value of 0 was applied for 0–5% staining, 1 for 5–25%, 2 for 25–50%, 3 for 50–75%, and 4 for 75–100% staining. All measurements were performed blinded to the source (NX or NX+BSA) of the section. Double Immunohistochemistry
Double-labeling experiments were performed to determine the spatial relationship between Kim-1 and MØ, -SMA, OPN, and vimentin. After endogenous peroxidase blocking, sections were incubated with a mixture of primary antibodies (Table 1), washed with PBS, and incubated with a mixture of peroxidase-conjugated goat anti-rabbit and alkaline phosphatase-labeled goat anti-mouse antibodies (DakoCytomation). Peroxidase activity was developed in DAB. Endogenous alkaline phosphatase was blocked with levamisole (Sigma). Specific alkaline phosphatase activity was developed with Naphtol AS-MX phosphate and Fast Blue BB (Sigma). Sections were counterstained with PAS. Appropriate isotype and PBS controls were consistently negative.
Western Blot Analysis
Ten slices of 10-µm frozen kidney tissue were homogenized in Krebs-Henseleit buffer. Insoluble material was pelleted by centrifugation (15 min at 20,000 g), resuspended in Krebs-Henseleit buffer, and repelleted by centrifugation. After being weighed, pellets were resuspended at 10 µl/mg in Krebs-Henseleit buffer containing 1% Triton X-100. Insoluble material was pelleted by centrifugation (15 min at 40,000 g), and the supernatant was collected. This supernatant contained the membrane protein fraction [adapted from Ichimura et al. (10)]. Total protein was measured using the Lowry method.
Aliquots of membrane protein fractions (20 µg mixed with 0.9% NaCl) were loaded on a 10% polyacrylamide gel, electrophoresed, and transferred onto polyvinylidene difluoride membranes in 25 mM Tris, 192 mM glycine, and 20% methanol. Blots were blocked 1 h in TBS containing 5% skim milk solution and 0.05% Tween 20 and probed with 2 ml of Kim-1 antibodies (peptide 9, concentration 0.5 µg/ml) in blocking solution. After washes with TBS containing 0.05% Tween 20, secondary probing was done with peroxidase-labeled goat anti-rabbit antibodies (1:1,000) diluted in blocking solution. Reactive bands were visualized by chemiluminescence with BM Chemiluminescence Blotting Substrate (POD, Roche).
Statistical Analysis
Data are presented as means ± SD. Statistical analyses were performed with SPSS Version 11.0. Differences between experimental (NX+BSA) and control (NX) groups were analyzed with independent sample t-tests. Correlations were assessed by linear regression analysis. Controls were not included in these analyses. A two-sided P value <0.05 was considered statistically significant.
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RESULTS |
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TOPABSTRACTMATERIALS AND METHODSRESULTSDISCUSSIONGRANTSREFERENCES |
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Clinical and pathological parameters are presented in Table 2. All NX+BSA rats developed massive proteinuria compared with NX (1,217 ± 313 vs. 18 ± 2 mg/day, P < 0.001). Kidney weight was almost doubled in NX+BSA compared with NX rats (4.1 ± 0.7 vs. 2.3 ± 0.3 g, P < 0.001), whereas total body weight did not differ. Plasma albumin, cholesterol, and triglycerides were elevated in NX+BSA vs. NX rats; plasma glucose and creatinine clearance did not differ between the two groups.
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-SMA). Also, tubular OPN was markedly induced in NX+BSA.
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Semiquantitative RT-PCR revealed low levels of Kim-1 mRNA in the kidneys removed at nephrectomy (i.e., before the study) and in saline-injected NX kidneys (Fig. 1). In NX+BSA Kim-1 mRNA levels were upregulated eightfold compared with both the kidneys removed at nephrectomy and NX kidneys (both P < 0.001). Using in situ hybridization, traces of Kim-1 mRNA were found in a cluster of morphologically unaffected cortical tubules of NX kidneys (Fig. 2A). In contrast, in NX+BSA rats Kim-1 mRNA was abundantly expressed in a typical cytoplasmic staining pattern in dilated tubules in fibrotic areas throughout the entire cortex (Fig. 2B). In addition, some morphologically intact cortical proximal tubules were Kim-1 positive as well. Kim-1 was often present in a heterogeneous expression pattern within one cross-sectional tubular structure, with Kim-1-positive and -negative tubular cells adjacent to each other (Fig. 2C). Dilated tubules with fully denuded tubular membranes and shrunken cells were Kim-1 negative. Occasionally, tubular structures in the medulla showed Kim-1 mRNA expression.
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Kim-1 protein expression was undetectable in the kidneys removed at nephrectomy before the study, whereas immunohistochemistry sporadically revealed Kim-1-positive cortical tubules in NX rats (Fig. 2E). Kim-1 protein expression was massively upregulated in NX+BSA compared with NX rats (2.33 ± 1.07 vs. 0.39 ± 0.11% staining/field, P < 0.001; Fig. 1B). In NX+BSA kidneys, Kim-1 protein expression was predominantly located in the outer medulla, with focal cortical extensions. Single dilated nephron segments with flattened epithelium from outer medulla to the outer cortex were often positive (Fig. 2F). Protein expression was localized to the apical part of dilated tubules in fibrotic areas, with occasionally diffuse cytoplasmic staining. Kim-1-expressing dilated tubules often possessed a thickened or disrupted basement membrane and no visible cellular brush border. Besides Kim-1 expression in dilated tubules, less pronounced, primarily apical, Kim-1 expression was found in some morphologically intact proximal tubules. Consistent with the in situ hybridization results, we often noted a heterogeneous Kim-1-staining pattern between individual cells within one cross-sectional dilated tubular structure (Fig. 2G). The renal papilla, glomeruli, and tubular casts were negative.
Kim-1 Western Blotting
For further quantifications of Kim-1 protein expression after protein overload, membrane fractions of kidney homogenates from NX and NX+BSA were analyzed. In NX+BSA rats, besides a 50-kDa protein that was also present in NX, two additional protein bands were seen with a molecular mass of 
40 and 70–80 kDa (Fig. 3), corresponding to previous results by Ichimura et al. (10). These bands possibly represent different degrees of glycosylation (10).
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At baseline, low levels of urinary Kim-1 protein were found. After protein-overload induction, urinary Kim-1 was significantly higher in NX+BSA than in NX controls at all measured time points (Fig. 4). The amount of urinary Kim-1 at week 3 correlated with Kim-1 tissue expression (r = 0.66, P = 0.02) and proteinuria (r = 0.63, P = 0.04).
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Kim-1 related to tubulointerstitial damage.
To characterize tubular Kim-1 expression in relation to classic markers of interstitial inflammation and fibrosis, we compared Kim-1 expression to MØ infiltration and -SMA expression. Double-labeling immunohistochemistry revealed that Kim-1-positive tubules were associated with aggregates of MØ and areas with increased -SMA expression (Fig. 5, A and C). There was a clear correlation between Kim-1 expression and interstitial MØ (r = 0.95, P < 0.001) and interstitial -SMA (r = 0.67, P = 0.001; Fig. 5, B and D).
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Double labeling revealed a spatial relationship between OPN and Kim-1. In tubulointerstitial fibrotic areas, virtually all dilated tubules expressing Kim-1 were also OPN positive (Fig. 5E). In these tubules, Kim-1 is expressed at the apical membrane whereas OPN expression is predominantly cytoplasmatic (Fig. 5F). Furthermore, OPN but not Kim-1 expression was found in morphologically unaffected tubules directly surrounding Kim-1/OPN double-positive tubules. A clear correlation between tubular Kim-1 and OPN expression was found (r = 0.92, P < 0.001).
Double labeling for Kim-1 and vimentin revealed a mosaic tubular staining pattern in areas with tubulointerstitial damage. Vimentin was expressed in extremely damaged tubular structures at the luminal and lateral side of the cell. However, only a few tubular cells expressed both Kim-1 and vimentin, and tubular structures with less pronounced damage expressed Kim-1 only (Fig. 5, G and H).
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DISCUSSION |
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TOPABSTRACTMATERIALS AND METHODSRESULTSDISCUSSIONGRANTSREFERENCES |
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In this study, we describe Kim-1 in acute proteinuria-induced renal damage. Kim-1 induction has been demonstrated after ischemic (10, 18) and nephrotoxic (11) renal injury, in patients with acute ischemic tubular necrosis (9), and in renal cell carcinoma (8). In agreement with studies in ischemia-reperfusion (10, 18) Kim-1 was predominantly expressed in dilated and flattened cortical tubules. Similar to other studies (9–11), we primarily found Kim-1 localized to the apical part of the cell with occasionally a cytoplasmic staining pattern. The mosaic staining pattern within one tubular cross section resembles Kim-1 expression after folic acid- and cisplatin-induced renal injury (11) and in cystic kidneys (14), although it was absent after transient ureteral obstruction (14). As in nephrotoxic renal injury (11), ischemic acute tubular necrosis (9), and renal cell carcinoma (8), we also found high urinary Kim-1 after proteinuria-induced renal damage. Moreover, urinary Kim-1 levels during acute proteinuria correlated with Kim-1 tissue expression.
Although the present study does not provide evidence on the trigger(s) for Kim-1 induction, various mechanisms could be involved. First, protein-overload nephropathy is associated with activation of PTC by a tubulotoxic ultrafiltrate, and subsequent production of proinflammatory and profibrotic mediators, which initiate tubulointerstitial damage (4, 5, 7). PTC in vitro exposed to high concentrations of proteins present in the ultrafiltrate of nephrotic patients, show increased synthesis of cytokines/chemokines, such as MCP-1, RANTES, IL-8, endothelin-1, and TGF- (27). Kim-1 induction might well be part of that general pathway leading from initial tubular activation to chronic damage caused by extended exposure to the tubulotoxic ultrafiltrate.
In addition to the role of the tubulotoxic ultrafiltrate, lack of oxygen might also be involved in Kim-1 induction. Kim-1 expression was first noted in rats after ischemic injury in corticomedullary areas, the most vulnerable site for oxygen deprivation (10), and in patients with ischemic acute tubular necrosis (9), which led these authors to suggest that ischemia/hypoxia is a major trigger for Kim-1 induction. However, in murine polycystic kidney disease, Kim-1 is upregulated without signs of ischemic injury (14). In our model, tubular protein overloading could lead to loss of tubulointerstitial perfusion caused by edema or loss of peritubular capillaries (3). Cytokines and growth factors produced by activated tubular cells cause interstitial changes such as fibrosis and MØ accumulation. This process may cause damage to the capillary endothelium and/or activate interstitial fibroblasts to produce extracellular matrix. These local processes may hamper oxygen supply to adjacent tubular cells, known to be extremely vulnerable to oxygen deprivation. Furthermore, a tubular disbalance in energy expenditure and availability might also result in tubular ischemia, because tubular protein overloading leads to an increased lysosomal processing (13), affecting oxygen demand.
The third possible mechanism for induction of Kim-1 is tubular obstruction by cast formation. In protein overload, the formation of protein casts and the subsequent tubular obstruction, mechanical stress, and increased glomerular pressure may activate tubular cells, leading to Kim-1 induction. Kim-1 structurally resembles mucosal addressin cell adhesion molecule-1 (1). It is possible that Kim-1 is involved in surface adhesion interactions and possibly cast formation. However, in our model tubular casts were not related to Kim-1 expression, as was seen in nephrotoxic injury (11), which makes it unlikely that cast formation only triggers Kim-1 induction. As Kim-1 expression is seen in different situations and models, it is most likely that induction of Kim-1 is dependent on an interplay of different factors, leading to tubular cell stress and activation.
OPN, vimentin, and Kim-1 showed a focal expression pattern, indicating that not all nephrons are damaged to the same extent. Apparently, nephrons are unequally vulnerable to damage and/or exposed to unequal amounts of tubulotoxic ultrafiltrate. Also, cells may respond in different ways to injury: uninjured cells proliferate and repopulate damaged nephron segments with new cells. Nonlethally damaged cells recover, and some damaged cells may undergo cell death by apoptosis or necrosis (19). Because all different stages are present after injury, this probably explains the focal distribution of damage and the heterogeneous Kim-1 expression between and within tubular structures.
In response to injury, tubular cells express various proteins. We found OPN-positive, morphologically unaffected, tubular structures that did not stain for Kim-1 surrounding areas with severe fibrosis and coexpression of tubular OPN and Kim-1. This suggests that in early stages of damage OPN expression may precede Kim-1 expression. After OPN and Kim-1 expression, the PTC may either undergo apoptosis/necrosis or develop into a nonmature, dedifferentiated vimentin-positive tubular cell. Dedifferentiated vimentin-positive cells can proliferate and restore the tubular structure (2). It has also been proposed that these cells can transform from an epithelial to mesenchymal cell type (EMT) and migrate as fibroblasts into the tubulointerstitium and contribute to fibrosis (12). Thus vimentin-positive cells are important in restoration of tubular structures. Kim-1 colocalized with vimentin after ischemia-reperfusion (10) and S-(1,1,2,2-tetrafluoroethyl)-L-cysteine-induced renal injury (11). After folic acid- and cisplatin-induced injury, Kim-1 was expressed in the absence of detectable vimentin staining, whereas in a later phase coexpression of Kim-1 and vimentin increased (11). In our study, we only found scarce colocalization, with vimentin predominantly expressed in more damaged and Kim-1 in less damaged tubular areas. This may suggest a sequential or damage-dependent expression of these two markers, which can only be proved by sequential analyses in times earlier in the model.
Kim-1 is induced after various types of injury, and both tissue and urinary Kim-1 expression can serve as markers for renal damage (9, 11). However, the function of Kim-1 remains unclear. Kim-1 might either actively modulate tubulointerstitial injury as has been proposed (14) or be a consequence of tubulointerstitial injury. Structurally, Kim-1 resembles an adhesion molecule, and human KIM-1 is also known as hepatitis A virus cellular receptor (6, 23) and T cell immunoglobulin, mucin-like domain 1 (TIM-1) (15, 17). TIM-1 is expressed on T cells, and in mice it was demonstrated that Tim-4 is the natural ligand for Tim-1 (16). This suggests that Kim-1 might also interact with other protein(s). Intriguingly, the extracellular part of Kim-1 can be shed into the tubular lumen, and this ectodomain shedding is metalloproteinase driven (26). In vivo the Kim-1 ectodomain may form a protective layer on the proximal tubular cells, thereby protecting them from protein casts that are formed within the tubular lumen. Kim-1 may also prevent the formation of tubular casts. Although the pathophysiological implications of Kim-1 shedding are unclear, it can be used as a urinary biomarker (8, 9).
In conclusion, Kim-1 is markedly induced in proteinuric renal disease. Expression is largely restricted to tubular cells in areas with tubulointerstitial damage, suggesting a modulatory role in renal damage. Based on its colocalization with OPN, but limited association with epithelial dedifferentiation, we hypothesize that Kim-1 induction is an intermediate step in the sequence of events progressing from primary tubular activation to end-stage tubulointerstitial damage. Urinary Kim-1 levels correlate with renal Kim-1 expression, and thus Kim-1 may be used as a relevant biomarker for proteinuria-induced renal damage. The exact functional role of Kim-1 in proteinuria-induced tubulointerstitial damage remains to be elucidated.
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DISCLOSURES |
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ACKNOWLEDGMENTS |
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These data were presented at the 38th Annual Meeting of the American Society of Nephrology, Philadelphia, PA, November 8–13, 2005.
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FOOTNOTES |
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The costs of publication of this article were defrayed in part by the payment of page charges. The article must therefore be hereby marked "advertisement" in accordance with 18 U.S.C. Section 1734 solely to indicate this fact.
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) and NX+BSA (
), respectively. After unilateral nephrectomy (week 0; w0), urinary Kim-1 levels were low. After induction of protein overload (wk 1–3), urinary Kim-1 levels were significantly elevated in kidneys from NX+BSA rats compared with NX (all P < 0.05).