Circulating alpha-klotho levels are not disturbed in patients with type 2 diabetes with and without macrovascular disease in the absence of nephropathy
© van Ark et al.; licensee BioMed Central Ltd. 2013
Received: 22 May 2013
Accepted: 12 August 2013
Published: 14 August 2013
The Erratum to this article has been published in Cardiovascular Diabetology 2013 12:120
Diabetes is associated with a high incidence of macrovascular disease (MVD), including peripheral and coronary artery disease. Circulating soluble-Klotho (sKlotho) is produced in the kidney and is a putative anti-aging and vasculoprotective hormone. Reduced Klotho levels may therefore increase cardiovascular risk in diabetes. We investigated if sKlotho levels are decreased in type 2 diabetes and associate with MVD in the absence of diabetic nephropathy, and whether hyperglycemia affects renal Klotho production in vitro and in vivo.
sKlotho levels were determined with ELISA in diabetic and non-diabetic patients with and without MVD, and healthy control subjects. Human renal tubular epithelial cells (TECs) were isolated and exposed to high glucose levels (15 and 30 mM) in vitro and Klotho levels were measured with qPCR and quantitative immunofluorescence. Klotho mRNA expression was quantified in kidneys obtained from long term (3 and 8 months) diabetic Ins2Akita mice and normoglycemic control mice.
No significant differences in sKlotho levels were observed between diabetic patients with and without MVD (527 (433–704) pg/mL, n = 35), non-diabetic MVD patients (517 (349–571) pg/mL, n = 27), and healthy control subjects (435 (346–663) pg/mL, n = 15). High glucose (15 and 30 mM) did not alter Klotho expression in TECs. Long-term hyperglycemia in diabetic Ins2Akita mice (characterized by increased HbA1c levels [12.9 ± 0.3% (3 months) and 11.3 ± 2.0% (8 months)], p < 0.05 vs. non-diabetic mice) did not affect renal Klotho mRNA expression.
These data indicate that sKlotho levels are not affected in type 2 diabetes patients with and without MVD. Furthermore, hyperglycemia per se does not affect renal Klotho production. As type 2 diabetes does not alter sKlotho levels, sKlotho does not seem to play a major role in the pathogenesis of MVD in type 2 diabetes.
KeywordsAtherosclerosis Coronary artery disease Klotho Macrovascular disease Peripheral artery disease Type 2 diabetes
Patients with type 2 diabetes have a high incidence of macrovascular disease (MVD), including coronary artery disease (CAD) and peripheral artery disease (PAD) . The transmembrane protein αKlotho (referred to as Klotho) is predominantly expressed in renal distal tubular epithelial cells where it functions as an obligate co-receptor with Fibroblast Growth Factor Receptor 1 (FGFR1) for Fibroblast Growth Factor 23 (FGF23), a phosphaturic hormone essential for maintaining mineral homeostasis . In mice, Klotho deficiency is associated with accelerated and enhanced development of vasculopathy . The extracellular domain of Klotho can be cleaved and shed in the circulation (i.e. soluble Klotho [sKlotho]) where it may function as a vasculoprotective hormone possibly by enhancing endothelial function [4, 5] or direct inhibition of vascular calcification . Recently, in agreement with this, higher sKlotho levels appeared to be independently associated with reduced prevalence of cardiovascular disease . Moreover, in patients with chronic kidney disease (CKD) a graded reduction of urinary sKlotho has been described starting at an early stage of CKD, rendering sKlotho as a sensitive biomarker for early detection of CKD [6, 8]. Finally, a reduction in renal Klotho gene expression has been observed in kidneys from patients with diabetic nephropathy .
Studies on sKlotho levels in diabetes are scarce and inconclusive and data have been obtained using various commercially available assays [10, 11]. We need to interpret these data with caution, because a reliable ELISA-based assay to measure sKlotho levels has only recently become available . Nevertheless, reduced sKlotho levels in type 2 diabetes could potentially be used as a biomarker for cardiovascular risk, and therefore studies on this are warranted. In addition, given its impact on both endothelial function and medial calcification, sKlotho may be involved in the pathogenesis of MVD in type 2 diabetes.
Against this background, in the current cross-sectional study we determined serum sKlotho levels in patients with type 2 diabetes with and without MVD, but without diabetic nephropathy. In addition we investigated the potential effect of hyperglycemia on renal Klotho expression. The following hypotheses were tested: 1) type 2 diabetes is associated with reduced sKlotho levels, particularly in patients with MVD and 2) hyperglycemia reduces renal Klotho expression. To this end, sKlotho ELISAs on patient sera were performed as well as in vivo mouse and in vitro cell culture experiments. Our data indicate that sKlotho levels are not affected in type 2 diabetic patients with and without MVD. This is supported by our in vivo and in vitro data showing that hyperglycemia per se does not affect renal Klotho production.
Patients with type 2 diabetes and non-diabetic subjects with and without MVD were included in this study. Individuals included are a subset of subjects on which we recently reported . Patients were assigned to the following groups: diabetes, no MVD (n = 11); diabetes with CAD (n = 12); diabetes with PAD (n = 12); no diabetes with CAD (n = 13); and no diabetes with PAD (n = 14). Diagnosis of type 2 diabetes was based on criteria recommended by the WHO (http://whqlibdoc.who.int/publications/2006/9241594934_eng.pdf). In addition, age and sex-matched healthy control subjects (n = 15) were included in the study. Diagnosis of CAD was based on prior myocardial infarction (> 6 months), or of evidence of significant coronary artery stenosis during angiography. PAD was diagnosed based on a history of claudication or rest pain and assessed with bilateral peripheral arterial foot pulse examination and duplex ultrasonography. Patients with clinical evidence of both CAD and PAD were excluded from the study. Patients with clinically documented nephropathy (with eGFR < 60 mL/min/1.73 m2 or macroalbuminuria) were excluded from the study to exclude the potential confounding effect of kidney disease on sKlotho levels and presence of arterial disease. Additional exclusion criteria were: retinopathy, auto-immune diseases, neoplasms, acute or chronic infections, recent (< 6 months) surgery, age >80 yrs, hemodialysis and use of immunosuppressive agents. Participants were screened for cardiovascular risk factors including smoking, hypertension and BMI. In addition, laboratory measurements for glucose, HbA1c, lipid levels, blood urea nitrogen (BUN), serum creatinine, serum phosphate and serum calcium were performed. Estimated glomerular filtration rate (eGFR, mL/min per 1.73 m2) was calculated using the Chronic Kidney Disease Epidemiology Collaboration (CKD-EPI) equation . Blood samples were obtained by venipuncture and collected in EDTA vacutainers for plasma isolation and in coagulation tubes for isolation of serum. Coagulation tubes were allowed to clot for a minimum of 30 minutes at room temperature before serum separation. Blood samples were centrifuged and plasma or serum was collected and stored at −80°C until further analysis. All participants gave written informed consent. The study protocol was approved by the local ethics committee of the University Medical Center Groningen (METc: 2008/335) and investigations were carried out in accordance with the principles of the Declaration of Helsinki.
Spontaneous diabetic Ins2Akita mice
Spontaneous diabetic heterozygous Ins2Akita+/− (Ins2Akita) mice, purchased from Jackson Laboratory (Charles River Laboratories, Sulzfeld, Germany), were bred at the animal facility of the University Hospital Mannheim, University of Heidelberg. Age-matched non-diabetic homozygous Ins2Akita−/− littermates served as control. Mice were housed in groups in cages with free access to standard food and water under a 12-h light and 12-h dark rhythm. Both male and female mice were used in this study. Glucose levels and body weight were monitored consecutively every other week, and HbA1c concentration was determined by affinity chromatography at the end of the study (MicromatII; Bio-Rad Laboratories, Munich, Germany). Insulin was occasionally given to individual diabetic mice to prevent critical weight loss. After 3 and 8 months of diabetes, kidneys were harvested under deep anesthesia and immediately frozen at −80°C until further analysis. Animal experiments were performed according to the ‘Principles of laboratory animal care’ (NIH publication no. 85–23, revised 1985; http://grants1.nih.gov/grants/olaw/references/phspol.htm) and were approved by the Institutional Animal Care and Use Committee of the University of Heidelberg.
Klotho and cFGF23 ELISA
sKlotho levels were determined in human serum using a sandwich ELISA (Immuno-Biological Laboratories, Takasaki, Japan) with an intra-assay coefficient of variation (cv) and interassay cv of < 5% and < 8% respectively. c-Terminal FGF23 levels were determined in plasma using a sandwich ELISA (Immutopics, San Clemente CA) with an intra-assay cv of < 5% and interassay cv of < 16% . Both assays were performed according to the manufacturer’s instructions. All samples and standards were measured in duplicate. Absorbance values were measured at 450 nm with a VarioSkan Microplate Reader (Thermo Scientific, Landsmeer, The Netherlands).
Primary tubular epithelial cell (TEC) culture
TECs were isolated from a segment of healthy renal cortex, which was obtained from a nephrectomized kidney with renal cell carcinoma. The segment was taken distal from the tumor. The segment was cut into 1 mm3 pieces, washed in HBSS and subsequently placed in a T25 culture flask coated with FBS. The fragments were allowed to attach by putting the flask upside down for 1 hour at 37°C, 5% CO2. Next, 2.5 mL TEC medium (DMEM/Ham-F12 1:1 supplemented with Penicillin/Streptomycin, 25 mM HEPES, 2 mM L-glutamine, insulin-transferrin-sodium selenite supplement, hydrocortisone (36 ng/ml), epidermal growth-factor (10 ng/ml) and 5% heat-inactivated FBS) was gently added to the flask which was then put right-side-up in the incubator. Explant cultures were left untouched for 3 days after which 1 mL medium was added every 2–3 days. After 21 days, detached floating tissue fragments were removed and adherent TECs were detached using Trypsin/EDTA and seeded in new flasks (passage 1). Medium wash refreshed every 2–3 days.
Immunostaining was performed on TECs (passage 2) cultured in 8-well permanox chamber slides (Nalge Nunc, Creek Drive, USA). Subconfluent monolayers were washed with PBS and fixed for 15 minutes (room temperature) with 2% paraformaldehyde in PBS. After fixation, cells were washed twice with PBS and subsequently permeabilized in PBS/0.05% Triton for 3 minutes and washed with PBS. Next, cells were incubated with primary antibodies diluted in PBS/1% BSA for 60 minutes at room temperature. The following primary antibodies were used: mouse anti-cytokeratin (Clone AE1/AE3, DAKO, Glostrup, Denmark), mouse anti-cytokeratin 7 (Clone OV-TL 12/30, DAKO), mouse anti-epithelial membrane antigen (EMA, Clone E29, DAKO), and rat anti-Klotho (Clone KM2076, Transgenic Inc., Tokyo, Japan). For immunofluorescence, cells were subsequently incubated (30 minutes, room temperature) with species-specific AlexaFluor®555 conjugated-secondary antibodies (Life Technologies) diluted in PBS/1% BSA containing DAPI for nuclear counterstaining. Slides were mounted with Aqua PolyMount (Polysciences, Warrington, USA). Images were acquired with a Zeiss AxioObserver Z1 inverted microscope equipped with TissueFAXS acquisition software (Tissuegnostics, Vienna, Austria). For Klotho immunohistochemistry, cells were incubated for 30 minutes at room temperature with horseradish peroxidase (HRP)-conjugated rabbit anti-rat antibodies, which was followed by incubation with HRP-conjugated goat anti-rabbit antibodies for 30 minutes at room temperature. Peroxidase staining reaction was developed with 3-Amino-9-ethylcarbazole (AEC) as substrate. Nuclear counterstaining was performed with Mayer’s haematoxilin. Slides were mounted with Kaiser’s glycerin and images were aquired with an Olympus BX50 microscope.
TEC stimulation and quantitative immunofluorescence
For in vitro stimulation experiments, TECs were seeded at a density of 2x104 cells/cm2 in TEC medium containing 0.5% FBS and were allowed to attach for 24 hours. For hyperglycemic conditions, TECs were subsequently incubated for 96 hours in TEC medium containing 0.5% FBS and 7.8 mM (standard concentration), 15 mM or 30 mM D-glucose. Medium was refreshed every day. For stimulation with human serum, cells were seeded as described above. After 24 hours attachment the medium was replaced with TEC medium containing 5% 0.22 μm filtered human serum derived from 5 diabetic patients without MVD (average serum glucose level 6.5 mmol/L) or 5 healthy control subjects (average serum glucose level 5.2 mmol/L). TECs were incubated for 96 hours and medium was replaced every day. Next, cells were either fixed in 2% paraformaldehyde for quantitative immunofluorescence or lysed in RLT buffer (Qiagen, Venlo, the Netherlands) and stored in −80°C for subsequent RNA isolation.
To quantify Klotho protein expression in vitro, we performed Klotho immunofluorescence asdescribed above followed by quantitative TissueFAXS analysis. The total number of cells per mm2 surface area as well as the percentage Klotho+ cells and staining intensity under each experimental condition were determined using the TissueFAXS system (Tissuegnostics, Vienna, Austria), as described before . To quantify the relative Klotho staining intensity, the mean fluorescence of intensity ratio (MFIR) was calculated by dividing the mean fluorescence intensity (MFI) of Klotho positive cells by the MFI of negative controls.
Quantitative real-time PCR
Total RNA was isolated from mouse kidneys and human TECs using the RNeasy Micro kit (Qiagen) according to the manufacturer’s instructions. The RNA quantity was measured with a Nanodrop spectrophotometer. For cDNA synthesis, 1 ug RNA was converted to cDNA using SuperScript II reverse transcriptase and random hexamere primers (Life Technologies) according to the manufacturer’s instructions. Klotho mRNA expression was measured with a Taqman Gene expression assay (Applied Biosystems, Carlsbad, USA) using exon junction spanning primers for human Klotho (assay Hs00183100_m1) and mouse Klotho (assay Mm00502002_m1). For normalization of mouse Klotho expression, B2M (Mm00437762_m1) was included as a housekeeping gene. For normalization of human Klotho expression, HPRT was included as a housekeeping gene using in house developed primers (FW: GGCAGTATAATCCAAAGATGGTCAA; REV: GTCTGGCTTATATCCAACACTTCGT) and probe (CAAGCTTGCTGGTGAAAAGGACCCC) (Eurogentec Nederland B.V., Maastricht, The Netherlands). PCR reactions were performed on a LightCycler 480 II Real-Time PCR System (Roche Applied Sciences, Penzburg, Germany). Gene expression was analyzed with LightCycler 480 Software release 1.5.0 (Roche). To obtain the ΔCt, the Ct values of the respective housekeeping gene were subtracted from the Klotho Ct value. We used the comparative Ct method (2-ΔCt method) to calculate relative Klotho gene expression.
Normal distribution of continuous variables was tested with the Shapiro-Wilk test. For normally distributed data, the unpaired two-tailed Student’s t-test was used for comparisons between two groups and the one-way ANOVA with Bonferroni post-hoc was used for comparisons between three or more groups. For non-normally distributed data the non-parametric Mann–Whitney U test was used for comparisons between two groups. For comparisons between three or more groups of non-normally distributed data, the Kruskall-Wallis one-way analysis of variance was performed followed by pairwise comparisons using the Mann–Whitney U test with Bonferroni multiple testing correction. Dichotomous patient characteristics were compared with the χ 2 test. Differences were considered significant at p < 0.05. Normally distributed data are reported as mean ± SEM, non-normally distributed data are reported as medians with interquartile range and categorical variables are presented as percentages. All data were analyzed using SPSS (version 20) and GraphPad Prism software (version 5).
No MVD (n = 11)
CAD (n = 12)
PAD (n = 12)
Healthy control (n = 15)
CAD (n = 13)
PAD (n = 14)
70.5 ± (63.5-74.0)
p < 0.05
Sex (% male)
Body mass index (kg/m2)
32.6 ± 2.6c
32.2 ± 2.1c
28.5 ± 3.1
24.5 ± 0.8
27.1 ± 1.0
23.6 ± 0.9
p < 0.001
Diabetes duration (years)
14.2 ± 1.0
16.8 ± 1.5d
11.3 ± 1.6
p < 0.05
p < 0.05
WBC count (106/mL)
p < 0.05
7.1 ± 0.4f
9.7 ± 1.5f
9.5 ± 1.5f
5.3 ± 0.1
6.0 ± 0.6
p < 0.001
HbA1c - (%)
p < 0.001
p < 0.001
p < 0.01
p < 0.05
p < 0.01
eGFR (mL/min/1.73 m2)
1.1 ± 0.1
1.2 ± 0.1
1.4 ± 0.1
1.2 ± 0.1
1.3 ± 0.1
1.4 ± 0.1
p < 0.001
ACE inhibitors (%)
p < 0.01
Angiotensin II inhibitor (%)
Alpha blockers (%)
Beta blockers (%)
p < 0.001
Calcium antagonists (%)
p < 0.01
p < 0.01
p < 0.001
Serum sKlotho and plasma cFGF23 levels
Effect of hyperglycemia and type 2 diabetic patient-derived serum on renal Klotho production
Renal Klotho mRNA expression in diabetic Ins2Akita mice
To study whether hyperglycemia affects renal Klotho expression in vivo, kidneys from 3 and 8 months hyperglycemic Ins2Akita mice were analyzed. Diabetic Ins2Akita mice had significantly increased HbA1c levels at both 3 months (13.1 (12.6-13.3)% (119.7 (114.2-121.9) mmol/mol) vs. 6.2 (6.0-6.6)% (44.3 (42.1-48.6) mmol/mol), p < 0.0001) and 8 months (10.9 (7.9-14.7)% (95.6 (62.3-137.2) mmol/mol) vs. 6.5 (5.4-6.6)% (47.5 (35.5-48.6) mmol/mol), p < 0.05) when compared with age-matched wild-type control mice, confirming a severe hyperglycemic state in diabetic Ins2Akita mice. No difference in renal Klotho gene expression in 3 and 8 months hyperglycemic Ins2Akita mice was observed when compared with age-matched normoglycemic control mice (Figure 3J). Ageing was clearly associated with significantly reduced Klotho gene expression (Figure 3J).
This study demonstrates that circulating sKlotho levels are similar in patients with type 2 diabetes and healthy individuals in the absence of nephropathy. In addition, no difference in sKlotho levels was observed between MVD patients and healthy control subjects, independent of the presence of diabetes. The lack of a decline in sKlotho in diabetic subjects with or without MVD can have several explanations. First, the null hypothesis might be true, implying that changes in sKlotho levels are not involved in the pathogenesis in MVD, independent from age or kidney function. Moreover, the widespread use of ACE-inhibitors and angiotensin receptor blockers in the diabetic subjects may have counterbalanced a presumed negative effect of diabetes on Klotho production . Finally, it has been shown that insulin promotes cleavage of Klotho from the plasma membrane by ADAM10 and ADAM17, generating sKlotho . Therefore, exogenously administered insulin in diabetic patients might compensate diabetes induced sKlotho depletion by increasing sKlotho shedding from the cell membrane. Our in vitro data are however not in favor of these explanations, but rather strengthen our conclusion that diabetes does not influence renal Klotho expression.
Our data are in contrast with results reported by Semba et al. showing that the presence of CVD is independently associated with reduced sKlotho levels . A potential explanation for this discrepancy might be that in the present study only patients with isolated CAD or PAD were included, while in the study by Semba et al. CVD patients with stroke and heart failure were included as well. Similar to our data, in the study by Semba et al. neither CAD nor PAD were separately associated with lower sKlotho levels.
Dysregulation of the FGF23-Klotho axis contributes to disturbed mineral homeostasis and as such might increase cardiovascular risk in diabetes. Therefore, we additionally measured cFGF23 levels in our cohort. However, like sKlotho, no differences in cFGF23 levels among the different study groups were observed. In line with this, serum calcium and phosphate levels were similar among all groups.
Circulating sKlotho concentration may not necessarily reflect total renal Klotho production, and despite similar sKlotho levels in diabetic and non-diabetic individuals, membrane-bound renal Klotho expression might be affected as a consequence of diabetes. Studies on this would have required kidney biopsy in our cohort. As a surrogate we performed in vitro experiments with TECs exposed to high glucose. In addition, we measured renal Klotho gene expression in long-term hyperglycemic Ins2Akita mice. Both the in vitro and in vivo mouse experiments revealed that renal Klotho production is not affected by hyperglycemia per se. Furthermore, the in vitro data suggest that circulating factors other than glucose in type 2 diabetes (such as glycated proteins or proinflammatory cytokines) do not influence renal Klotho production, as no difference in Klotho production between TECs exposed to serum derived from diabetic patients and healthy control subjects was observed.
Interpretation of results from different studies on sKlotho is still complicated by the fact that different assays (which are not all reliable and validated) are being used by different investigators. The results described here are in line with a recent study by Seiler et al. using the same Klotho assay, which showed that sKlotho levels are in fact not associated with deteriorated kidney function in CKD patients, and have poor predictive value for all-cause mortality after 2-years follow up. Furthermore, low sKlotho serum levels were not associated with an increased prevalence of diabetes in this study .
The present study is somewhat limited by a small sample size per group which may have obscured small differences in sKlotho levels between groups. Our in vitro studies were limited by the measurement of total cellular Klotho mRNA and protein under normo-and hyperglycemic culture conditions. We cannot exclude that the cleavage and excretion of sKlotho is affected by increased glucose levels in vitro.
Despite the recent interest in sKlotho as a biomarker for renal and cardiovascular disease, our study did not provide a rationale for using sKlotho levels as biomarker for MVD in type 2 diabetic patients and non-diabetic subjects in the absence of nephropathy. Based on our data, a major role of sKlotho in the pathophysiology of MVD in diabetes is unlikely.
A Disintegrin and metalloproteinase domain-containing protein
Blood urea nitrogen
Coronary artery disease
Chronic kidney disease
Estimated glomerular filtration rate
Epithelial membrane antigen
Fibroblast growth factor 23
Fibroblast growth factor receptor 1
Peripheral artery disease
Tubular epithelial cell
White blood cells.
The authors gratefully acknowledge the support A.C. Heijboer (Clinical Chemistry, VUmc) for performing cFGF23 ELISA. We thank R. Mencke for his help in performing Ca, P and BUN measurements. This study was supported by the Dutch Diabetes Foundation (grant 2006.01.007). Microscopical imaging was performed at the UMCG Imaging Center (UMIC), which is supported by the Netherlands Organisation for Health Research and Development (ZonMW grant 40-00506-98-9021).
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