Figures
Abstract
Nuclear receptor subfamily 1, group H, member 4 (Nr1h4, FXR) is a bile acid activated nuclear receptor mainly expressed in the liver, intestine, kidney and adrenal glands. Upon activation, the primary function is to suppress cholesterol 7 alpha-hydroxylase (Cyp7a1), the rate-limiting enzyme in the classic or neutral bile acid synthesis pathway. In the present study, a novel Fxr deficient mouse line was created and studied with respect to metabolism and liver function in ageing mice fed chow diet. The Fxr deficient mice were similar to wild type mice in terms of body weight, body composition, energy intake and expenditure as well as behaviours at a young age. However, from 15 weeks of age and onwards, the Fxr deficient mice had almost no body weight increase up to 39 weeks of age mainly because of lower body fat mass. The lower body weight gain was associated with increased energy expenditure that was not compensated by increased food intake. Fasting levels of glucose and insulin were lower and glucose tolerance was improved in old and lean Fxr deficient mice. However, the Fxr deficient mice displayed significantly increased liver weight, steatosis, hepatocyte ballooning degeneration and lobular inflammation together with elevated plasma levels of ALT, bilirubin and bile acids, findings compatible with non-alcoholic steatohepatitis (NASH) and cholestasis. In conclusion, ageing Fxr deficient mice display late onset leanness associated with elevated energy expenditure and improved glucose control but develop severe NASH-like liver pathology.
Citation: Bjursell M, Wedin M, Admyre T, Hermansson M, Böttcher G, Göransson M, et al. (2013) Ageing Fxr Deficient Mice Develop Increased Energy Expenditure, Improved Glucose Control and Liver Damage Resembling NASH. PLoS ONE 8(5): e64721. https://doi.org/10.1371/journal.pone.0064721
Editor: Carlos M. Rodriguez-Ortigosa, CIMA, University of Navarra, Spain
Received: November 29, 2012; Accepted: April 17, 2013; Published: May 20, 2013
Copyright: © 2013 Bjursell et al. This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Funding: The authors have no support or funding to report.
Competing interests: This study was funded by AstraZeneca, the employer of Mikael Bjursell, Marianne Wedin, Therése Admyre, Majlis Hermansson, Gerhard Böttcher, Melker Göransson, Daniel Linden, Krister Bamberg, Jan Oscarsson, Mohammad Bohlooly-Y. There are no patents, products in development or marketed products to declare. This does not alter the authors' adherence to all the PLOS ONE policies on sharing data and materials, as detailed online in the guide for authors.
Introduction
Nuclear receptors are ligand-activated transcription factors involved in a variety of physiological and developmental processes. Nuclear receptor subfamily 1, group H, member 4 (Nr1h4, Farnesoid X receptor (FXR)), is activated by bile acids and highly expressed in liver, kidney, adrenal glands and intestine [1], [2]. FXR is important for monitoring bile acid homeostasis and plays a central role in the regulation of lipid and glucose control [3]–[7]. Hepatic FXR is involved in a feedback inhibition loop regulating Cyp7a1 expression, where bile acid activated FXR up regulates the small heterodimer partner (SHP), an atypical nuclear receptor lacking a DNA binding domain. SHP suppresses Cyp7a1 expression by inhibiting liver receptor homologue 1 (Lrh-1), an obligate transcription factor for Cyp7a1 expression [8]. Intestinal FXR regulates bile acid synthesis via a pathway including up regulation of fibroblast growth factor (FGF) 15 in rodents and FGF19 in humans, which acts on liver FGF receptor 4 to suppress transcription of Cyp7a1 [9]–[11].
There are several previous reports describing effects of Fxr deficiency in mice. However, to our knowledge, only two Fxr deficient mouse lines have been described previously, one developed at Deltagen Inc. [12], [13], and one developed by Sinal et.al. [3]–[7], [9], [14]–[26]. The Deltagen derived Fxr deficient mouse line displays moderately elevated plasma bile salt levels, lower hepatic bile salt export pump (Abcb11) expression, slightly higher body and liver weight at 3 months of age together with lower fed and fasting blood glucose and changes in intestinal glucose absorption [12], [13]. The Fxr deficient mouse line originally derived from Sinal et.al. [5] has been more extensively studied and studies of this mouse model have shown the importance of Fxr for bile acid, lipid and glucose homeostasis, development of nephropathy, cancer and liver function in a variety of settings. Zhang and colleagues showed that Fxr deficient mice display unaltered fasting glucose but mild glucose intolerance and insulin resistance together with low hepatic levels of insulin stimulated IRS-2 phosphorylation [15]. Other studies on the Fxr deficient mouse line derived from Sinal et.al. reveal age dependent increase in fasting blood glucose, impaired glucose tolerance and attenuated peripheral glucose disposal as demonstrated by clamp studies [4], [7]. More recently, Fxr deficient mice bred on a leptin deficient genetic background displayed lower body weight and body fat mass together with lower blood glucose and insulin levels, improved glucose tolerance and insulin sensitivity, despite low energy expenditure [22]. In addition, Fxr deficient mice fed a high fat diet (HFD) also displayed lower body weight and plasma leptin levels together with low blood glucose, insulin and improved glucose tolerance [22] indicating that Fxr deficiency results in improved glucose control in obese animals. Also, Fxr deficiency bred on an Ldlr deficient background fed a HFD resulted in lower body weight at 3 months of age, dyslipidemia and elevated alanine transaminase (ALT) and alkaline phosphatase (ALP) levels. In addition, liver histopathology revealed mild macrosteatosis and focal inflammatory cell accumulation when Fxr/Ldlr deficient mice were fed chow diet, and severe macrosteatosis, hepatocyte ballooning, panlobular inflammation together with elevated hepatic expression of TNF-α and ICAM-1 when Fxr/Ldlr deficient mice were fed a HFD. The Fxr/Ldlr deficient mice were suggested to be a model displaying NASH [24]. FXR has also been reported to be important for liver regeneration and to prevent cell death [17], [18].
The present study aimed to further investigate the importance of a functional Fxr gene in the regulation of metabolism in a novel mouse line carrying a targeted deletion of the Fxr gene in order to evaluate FXR as a potential drug target. The aim of this study was to investigate the changes in energy metabolism in ageing Fxr deficient mice given ordinary low fat chow diet. In brief, we show that Fxr is of major importance for regulation of energy expenditure, glucose- and lipid metabolism and liver function in ageing mice even though they were not metabolically challenged.
Materials and Methods
Ethics Statement
All experiments were approved by Gothenburg Ethics Committee for Experimental Animals.
Generation of Fxr null mice
A Lox-P strategy was used to target the Nr1h4 (Fxr) locus in order to generate Fxr deficient mice. In essence, a 14.2 kb C57BL/6 mouse genomic sub clone was used as targeting vector, containing a floxed neomycin phosphotransferase selection marker cassette after the coding sequence in the untranslated region (UTR) and a single Lox-P site inserted in intron 8 of the Fxr locus (illustrated schematically in Fig. 1A). After linearization by XhoI, the targeting construct was electroporated into embryonic stem (ES) cells (derived from C57/J, Genome Systems, St. Louis, USA) and neomycin-resistant clones were selected in G-418-containing (300 µg/ml) media. Thus, the Fxr deficient mouse line was established on a pure C57BL/6 genetic background. Targeted clones were identified by PCR screening over the short arm homology of the construct and further confirmed by southern blot analyses using HindIII restriction enzyme (Fig. 1B). One clone was expanded and injected into BALB/C blastocysts to generate chimeric mice. Chimeric males were crossed to C57BL/6N female mice (Charles River, Sulzfeld, Germany) and genotyping of the black coat colour offspring was performed. The following primers were used to identify offspring with the targeted allele: forward neo-specific primer (F) 5′-GCTGACCGCTTCCTCGTGCTTT-3′ together with reverse primer within the short arm homology (R1) 5′-GGGAGAAGACTGCCACAGTTGA -3′. Heterozygous mice carrying Lox-P DNA sites were bred to ROSA26Cre mice [27] AstraZeneca in-house backcrossed more than 20 generation towards C57BL/6N (Charles River) in order to generate heterozygous Fxr deficient mice. The mice were identified using the following genotyping primers: intron specific: 5′-CCAGTGACCCGTGCCTGTAATGT -3′; intron specific; 5′- GGGAGAAGACTGCCACAGTTGA -3′ (627 bp products for the recombined allele and 2 253 bp products for the wild-type allele). Heterozygous Fxr deficient mice were intercrossed to generate homozygous Fxr animals, which proved to be viable.
(A) Schematic diagram of the Fxr gene and targeting vector. (B) Southern blot analyses of 8 targeted ES cell clones (lane 1–8) and a wild type control clone (lane 9), using HindIII restriction enzyme, resulting in wild type fragments of 10649 bp and targeted fragments of 13975 bp. (C) RT-PCR analyses of liver biopsies from WT (lane 1–2), Fxr heterozygous knock out (lane 3–4) and Fxr homozygous knock out (lane 5–6) mice. The RT-PCR products represent presence (lane 1–4) or absence (lane 5–6) of exon 9 in the Fxr gene.
To verify an Fxr null mutation, total RNA was prepared from livers of 12 weeks old homozygous, heterozygous, and wild-type littermates using the RNA STAT-60 Kit according to the manufacturer' instructions (Tel-Test Inc, Friendswood, USA). cDNA was synthesized using Superscript TM II RNAse H - Reverse Transcriptase and random hexamer primers (Life Technologies, Frederick, USA). RT-PCR was performed using the following primers: forward: Ex 5′-CTTGATGTGCTACAAAAGCTGTG-3′; reverse: Ex 5′-ACTCTCCAAGACATCAGCATCTC-3′ (Fig. 1C) to show exon 9 deletion in the Fxr deficient mice.
The Fxr heterozygous mouse colony was expanded by breeding to C57BL/6N (Charles River, Sulzfeld, Germany) and heterozygous intercross was performed to produce experimental (Fxr KO) and wild type (WT) littermate control cohorts, having a pure C57BL/6N genetic background. All experiments were performed using the same individuals of male mice over the course of the study.
Male Fxr KO and WT littermates were housed individually in a temperature controlled room (22°C) with a 12 hours light-dark cycle. They had access to normal chow diet (R36, Lactamin AB, Stockholm, Sweden) and water ad libitum. The R36 chow diet contained (weight%): 3.5% cellulose, (energy%): 22.9% protein, 67.1% carbohydrate and 9.6% fat. The main sources of proteins were from soy, grain and potatoes. Carbohydrate source was mainly grains and main fat source was soy. The energy density of R36 was 3.08 kcal/g.
The mice were initially studied in terms of gross appearance, cage side behaviours and basic responses, including assessment of balance, sensory pain, acoustic startle and grip strength (Grip strength meter, Columbus Instruments, Columbus, USA) as described previously [28]. To assess potential differences in behaviour in the Fxr KO mice, zero maze analysis was performed to investigate anxiety-like behaviours, passive avoidance to investigate memory and learning ability and forced swim test to study depression as described [28]. Open field locomotor behaviours were investigated during day time in specifically designed activity boxes (Kungsbacka mät-och reglerteknik, Kungsbacka, Sweden) as previously described [28].
Body weight, indirect calorimetry, locomotor activity and food intake
Body weight of the Fxr KO mice (n = 8) and WT mice (n = 8) were recorded on a weekly basis from 4 weeks of age up to 10 weeks of age and then biweekly from 15 to 30 weeks of age and finally at 39 weeks of age. Body length (nose to base of the tail) was assessed at, 3, 7, 9 and 30 weeks of age. Assessment of indirect calorimetry, food and water consumption and locomotor activity was performed in a CLAMS system (Columbus Instruments, Columbus, USA) at thermoneutral temperature (set for WT mice to be 29.5°C) as previously described [28]. The mice were placed in the CLAMS calorimeter chambers with ad libitum access to diet and water for 72 hours.
In older mice, food intake was analysed over 48 hours in food deprived mice (12 hours) as previously described [29] with a minor modification: no initial incubation (80°C for 1 hour) of the cages was done. Total faeces produced over the measurement periods were collected and energy content of the faeces was determined with a bomb calorimeter (C 5000, IKA® Werke GmbH & Co. KG, Germany) according to manufacturers protocol.
Body temperature and body composition
Rectal core body temperatures were recorded in conscious non-anaesthetised mice at day time (10.00–11.00 am) using a rectal probe [28]. Body composition was assessed by dual energy X-ray absorptiometry (DEXA, GE Lunar, Madison, USA) in isoflurane anaesthetised mice as previously described [28].
Oral glucose tolerance test (OGTT), blood- and tissue sampling
OGTT was performed in 30 weeks old Fxr KO and WT mice as previously described [29]. Homeostasis model assessment (HOMA) was calculated as [fasting blood glucose (mM) *fasting blood insulin (ng/ml)/22.5].
The mice were terminated at 39 weeks of age. Before sacrifice, the mice were fasted for four hours before measuring blood glucose levels (Accu-check device, Roche Diagnostics, Mannheim, Germany). The mice were then anaesthetised by isoflurane inhalation, euthanised by cardiac puncture and blood was collected in EDTA coated tubes by cardiac puncture. Blood plasma was separated by centrifugation (2500 rpm, 10 min. 4°C) and snap frozen in liquid nitrogen. The following organs and tissues were dissected and weighed: brain, caecum, liver, epididymal white adipose tissue (WAT), retroperitoneal WAT, interscapular brown adipose tissue (BAT), kidneys, spleen, testis, heart and gall bladder. Liver tissue samples were taken for hepatic triglyceride content analysis. Tissue samples of liver, epididymal WAT, interscapular BAT and skin were processed for histological analysis by immersion fixation in 4% buffered formaldehyde solution for 24–48 hours, dehydrated in graded series of alcohol and embedded in paraffin before sectioning.
Plasma analysis
Plasma levels of non-esterified fatty acids (NEFA), cholesterol, triglyceride, alanine aminotransferase (ALT), high density lipoprotein (HDL) and non-HDL cholesterol were determined as previously described [30]. Plasma levels of total bilirubin were measured using a colorimetric method (Kit No 11552414 216; BIL-T, Roche Diagnostics GmbH, Germany) and total bile acids were assessed by using an enzymatic method (Kit No Bl 3863, Randox Laboratoires Ltd, United Kingdom).
Expression levels analysis
RNA extraction, cDNA synthesis and quantification by Taqman real time PCR was performed as previously described [31]. Primer and probe sequences are presented in Table 1. Taqman assays for Cyp8b1 and Abcb11 were purchased as assay on demand (Applied Biosystems, Foster City, CA).
Histology
Epididymal WAT cell profile size, macrophage staining and quantification and interscapular BAT cell profile size and density was assessed in histological sections as previously described [30]. A histopathological examination and evaluation of epidermis and liver tissue samples was performed on routine hematoxylin- eosin stained sections and the degree of steatosis and inflammation was scored on a semi-quantitative 5 grade scale.
Statistical analysis
All values are given as group mean ± SEM. Comparison between two groups was done by Student' T-test. Parameters over time, e.g. energy expenditure and RER, were analysed by a mixed model 2-way ANOVA using the SPSS software. Values of p<0.05 were considered significant. The data were log normalised when appropriate.
Results
Animals
Fxr deficient mice (Fxr KO) were generated by targeted deletion of a 3326 bp DNA segment of the coding region of exon 9 (Fig. 1A) and positive ES cell clones identified by southern blot (Fig. 1B). To confirm absence of Fxr transcript in the Fxr KO mice, RT-PCR analysis of mRNA prepared from liver biopsies were performed. As expected, no expression of Fxr was observed in the Fxr KO mice (Fig.1C). Intercross of heterozygous Fxr mice resulted in offspring of normal litter sizes. Of the male offspring; 22% (n = 12) were homozygous, 58% (n = 32) were heterozygous and 20% (n = 11) were wild type mice. All experiments were performed on the same individuals of single housed male mice.
The mice were analysed in a battery of tests to assess appearance, cage side behaviours, basic responses and functions, anxiety, memory and learning and depression [28] between 4–11 weeks of age. No significant differences were observed between Fxr KO mice and WT mice with respect to any parameter investigated (data not shown) indicating that Fxr deficiency does not alter gross appearance or behaviour in mice. Locomotor behaviours were investigated in more detail in an open field locomotor activity setup. No significant differences in day-time locomotor behaviours were observed at 9 weeks of age between Fxr KO mice and WT mice.
Body weight and body composition
Body weight did not differ significantly between young Fxr KO and WT mice. From 21 weeks of age and onwards, the Fxr KO mice displayed significantly lower body weight compared to the WT control mice (Fig. 2). At termination (39 weeks of age), the Fxr KO mice displayed approximately 8 g lower body weight compared to the WT mice (WT: 39.2±2.1 g; Fxr KO: 30.9±1.7 g;−21%; p<0.01). Body length was not significantly different at any time point assessed between Fxr KO and WT mice (data not shown).
Body weight development over 39 weeks in WT (n = 8, black solid line) and Fxr KO mice (n = 8, grey dashed line). Statistical analysis was done by a repeated Student' T-test. * p<0.05 Fxr KO vs. WT mice.
Body composition was assessed at 9 weeks of age and then again at 30 weeks of age. At 9 weeks of age, no significant differences were observed in body lean mass, body fat mass or bone mineral content (BMC) between Fxr KO and WT mice (data not shown). However, bone mineral density (BMD) was slightly but significantly lower in the Fxr KO compared to WT mice (WT: 46.5±0.4 g/cm2; Fxr KO: 45.1±0.3 g/cm2, p<0.05). At 30 weeks of age, the Fxr KO mice displayed significantly lower BMD, BMC and body fat mass, whereas body lean mass was not significantly different between Fxr KO and WT mice (Table 2).
Energy intake, energy expenditure, locomotor activity and core body temperature
The mice were analysed with respect to energy intake, faecal energy output, energy expenditure, core body temperature and locomotor activity initially at a younger age and then again at an about 30 weeks of age.
At 8 weeks of age, no significant differences were observed in terms of energy intake, faecal energy density, total faecal energy, energy uptake (energy intake minus faecal energy) or water intake between the Fxr KO and WT mice (data not shown). No significant difference was observed in respiratory exchange ratio (RER), energy expenditure, core body temperature or spontaneous locomotor or rearing activity between Fxr KO and WT mice at that age (data not shown).
The mice were reanalyzed at 29–31 weeks of age. Total energy intake was not significantly different, whereas relative energy intake (relative to body weight) was significantly increased in the Fxr KO mice compared to WT mice (Table 3). Total water intake was not significantly different, whereas relative water intake (relative to body weight) was significantly higher in the Fxr KO compared to the WT mice (Table 3). Total faeces production, faeces energy density, total faecal energy output or energy uptake (energy intake minus energy lost in faeces) were not significantly different between Fxr KO and WT mice, whereas relative energy uptake (relative to body weight) was significantly increased in the Fxr KO compared to the WT mice (Table 3). When the parameters above were related to lean body mass, no significant differences were observed between Fxr KO and WT mice (data not shown).
Total energy expenditure (kcal/hr) was not significantly different, whereas energy expenditure related to body weight (Fig. 3A) and energy expenditure related to lean body mass (Fig. 3B) were significantly increased in the Fxr KO compared to the WT mice. No significant difference was observed in RER between Fxr KO and WT mice at this age (data not shown). Core body temperature was not significantly different between the experimental and control groups of mice (WT: 36.9±0.2°C; Fxr KO: 36.6±0.2°C, p NS). Total locomotor activity was not significantly different between Fxr KO and WT mice over the 72 hour indirect calorimetry analysis (data not shown).
(A) Energy expenditure relative to body weight assessed in kilocalories per hour and kilogram body weight (kcal/Hr/kg) and (B) energy expenditure relative to lean body mass (lbm) in WT (n = 8, black solid line) and Fxr KO mice (n = 8, grey dashed line). Black bars at the X-axis represent light off. Statistical analysis was performed using a 2 way ANOVA mixed model.
Oral glucose tolerance test
At 30 weeks of age, glucose tolerance was analyzed following 5 hour diet deprivation. The Fxr KO mice displayed significantly lower fasting glucose (−19%, p<0.01) and fasting insulin (−62% p<0.05) levels (Fig. 4) resulting in a 70% lower HOMA-IR index (WT: 0.52±0.15; Fxr KO: 0.16±0.03, p<0.05). Following an oral glucose challenge (2 g/kg), both the glucose and insulin response were significantly lower in the Fxr KO compared to the WT mice (Fig. 4). Glucose AUC was 26% lower (WT: 1568.6±64.4; Fxr KO: 1163.5±27.3, p<0.001) and insulin AUC was 58% lower (WT: 184.4±20.2; Fxr KO: 78.2±11.5, p<0.001) in the Fxr KO compared to the WT mice.
Oral glucose tolerance test in WT (n = 7, black solid line) and Fxr KO mice (n = 7, grey dashed line) mice. Statistical analysis of area under the curve (AUC) values was performed using Student's T-test.
Tissue weights and hepatic triglyceride content
The mice were sacrificed at 39 weeks of age and the tissue weights are collected in Table 4. At sacrifice it was noted that the liver, paws and plasma were yellow in colour in the Fxr KO mice, indicative of jaundice. The weight of the liver was increased by over 40% (Fig. 5A) and an even greater increase in liver weight was observed when related to individual body weights (WT: 42.5±2.9 mg/g body weight; Fxr KO: 79.8±6.6 mg/g body weight, p<0.001). Hepatic levels of triglycerides were significantly increased, both in term of absolute (Fig. 5A) and relative quantities (WT: 55.9±15.7 mg tg/g liver; Fxr KO: 91.9±6.8 mg tg/g liver, p<0.05). The non-emptied gall bladder had 5-fold higher weight in the Fxr KO compared to the WT mice (Fig. 5A) and relative to body weight the difference between the genotypes was even greater (WT: 0.36±0.04 mg/g body weight; Fxr KO: 2.50±0.77 mg/g body weight, p<0.01).
(A) Weight of liver, liver triglyceride (TG) content and weight of the gall bladder in WT (n = 8, black bars) and Fxr KO mice (n = 8, grey bars). Statistical analysis was performed using Student's T-test. ** p<0.01 Fxr KO vs. WT mice. (B) Representative slides of livers from WT (n = 8) and Fxr KO mice (n = 8) as indicated. The arrows indicate perisinusoidal/sinusoidal foam cells (FC), lobular inflammation (LI) and ballooning degeneration (BD).
Both absolute and relative (relative to body weight) weights of epididymal WAT, retroperitoneal WAT and interscapular BAT was significantly lower, whereas the weight of the spleen and caecum were significantly higher in the Fxr KO compared to the WT mice.
Plasma analysis
All data from the plasma analysis is collected in Table 5. At termination, fasting blood glucose levels were significantly lower in the Fxr KO compared to the WT mice. Plasma lipid analysis revealed significantly lower levels of non-esterified fatty acids (NEFA) and higher levels of total cholesterol and non-HDL cholesterol in the Fxr KO compared to the WT mice. Plasma levels of total bile acids were more than 30-fold higher in the Fxr KO compared to WT mice. Moreover, plasma levels of total bilirubin and alanine aminotransferase (ALT) were more than 20-fold and 4-fold higher respectively in the Fxr KO mice, indicating markedly deranged liver function.
Histology and liver expression analyses
Inferior lobes of the liver were sampled to assess liver histopathology. Livers from the Fxr KO displayed higher degree of steatosis, perisinusoidal/sinusoidal foam cells, ballooning degeneration and lobular inflammation compared to WT mice, indicative of liver dysfunction and NASH-like steatohepatitis in the Fxr KO mice (Fig 5B). To investigate possible mechanisms behind changes in liver metabolism of bile acids and lipids as well as liver inflammation, expression levels of a series of genes were assessed (Fig. 6). The Fxr KO mice displayed significantly increased hepatic expression of Cyp7a1 and Cyp8b1, but markedly lower expression of Abcb11 (bile acid export pump (BSEP)) (Fig. 6). PPARα and two down-stream target genes (medium-chain acyl-CoA dehydrogenase and acyl-CoA oxidase) were analysed to understand if increased PPARα signalling could help to explain the increased energy expenditure, liver size and triglyceride content [32], [33]. Expression level of Pparα mRNA was decreased (Fig. 6) whereas expression of medium-chain acyl-CoA dehydrogenase and acyl-CoA oxidase mRNA was not significantly different between the Fxr KO and WT animals (data not shown). Since liver triglyceride levels were increased, while plasma levels of fatty acids were reduced in Fxr KO mice as compared to WT controls, key genes involved in de novo fatty acid synthesis were analysed. Srebp-1c mRNA expression was lower in Fxr KO, while Fas and Scd-1 mRNA expression was not significantly different between the two groups of animals (data not shown). Heme oxygenase -1 (HO-1) mRNA expression was increased more than 2-fold in the Fxr KO livers indicating increased oxidative stress in the Fxr deficient livers. Tnfα, Ccl5/Rantes, Tlr-4 and Cd11c expression was higher in livers from Fxr KO mice than in WT mice indicating severe inflammatory changes (Fig. 6).
RNA expression levels in WT (n = 8, black bars) and Fxr KO mice (n = 8, grey bars). Statistical analysis was performed using Student's T-test. * p<0.05, ** p<0.01, *** p<0.001 Fxr KO vs. WT mice.
White adipose tissue (WAT) was analysed in terms of cell profile size and macrophage content in sections. Cell profile size distribution analysis of>5000 cells/animal indicated that adipocytes from the Fxr KO mice were significantly smaller in size compared to WT mice (Fig. 7A). WAT macrophage content analyses indicated less ‘crown like’ structures in the Fxr KO mice, however the quantification did not reveal a statistically significant difference between Fxr KO and WT mice (Fig. 7B). The density of the interscapular BAT depot was significantly higher in the Fxr KO mice, indicating decreased amount of lipid droplets in BAT from Fxr KO compared to WT mice (Fig. 7C). Skin samples were analysed for potential histopathological alterations of epidermis, but no histological skin abnormalities were detected, including no alterations in epidermal thickness or in dermal or epidermal appearance in the Fxr KO compared to WT mice (Fig. 8).
(A) Representative slides of basic fuchsin stained WAT from WT (n = 8) and Fxr KO mice (n = 8) as indicated. (B) Representative slides of WAT stained for Mac2 (Macrophage 2 antigen, Galectin-3) from WT (n = 8) and Fxr KO mice (n = 8) as indicated. (C) Representative slides of hematoxylin- eosin stained BAT from WT (n = 8) and Fxr KO mice (n = 8) as indicated. Statistical analysis was performed using Student's T-test. ** p<0.01 Fxr KO vs. WT mice.
Representative slides of skin biopsies from WT (n = 8) and Fxr KO mice (n = 8) as indicated.
Discussion
The Fxr deficient mice from this novel mouse line display reduced body weight gain from 21 weeks of age and onwards which is explained by increased energy expenditure. Moreover, the ageing Fxr deficient mice, without previous metabolic challenge, showed a picture of intrahepatic cholestasis and hepatocyte damage resembling non-alcoholic steatohepatitis (NASH). The livers were yellowish, steatotic and enlarged and plasma levels of ALT, bile acids and bilirubin were markedly elevated in the Fxr deficient mice. Also, the Fxr deficient mice were hypercholesterolemic, possibly as a consequence of the cholestasis. Towards the end of the study, the Fxr deficient mice displayed improved glucose tolerance and lower HOMA-IR index indicating improved insulin sensitivity.
In contrast to our results, it has been shown that Fxr deficient mice have reduced glucose tolerance and insulin resistance at 8–12 weeks of age [4] and 18–20 weeks of age [7]. Body weight gain was shown to be similar in Fxr deficient and WT mice up to 18–20 weeks of age, whereas body fat mass were reduced. The reduced body fat mass was explained by reduced adipocyte differentiation, and it was suggested that an increased flux of fatty acids to skeletal muscle reduced glucose tolerance and insulin sensitivity [7]. In contrast, ageing Fxr deficient mice fed a chow diet in the present study displayed reduced body fat mass and lower free fatty acids levels, indicating reduced flux of fatty acids from the adipose tissue. A later study investigated the effect of Fxr deficiency in mice fed high fat diet and on a leptin deficient genetic background [22]. In line with the present study, they found reduced body weight gain, body fat mass and smaller adipocytes. Moreover, they showed that Fxr deficiency improved glucose tolerance and insulin sensitivity in spite of increased liver fat [22]. Together with our results it is therefore likely that the improved glucose control in older Fxr deficient mice independent of genetic background is explained by lower body weight gain and fat mass. In contrast to our findings of increased energy expenditure as an explanation to the reduced body weight gain, the Fxr deficient mice on the leptin deficient background displayed reduced energy expenditure, and a trend towards decreased food intake [22]. We extended these previous studies by showing that improved glucose control as a result of Fxr deficiency does not only occur after diet induced or genetically induced obesity, but also in association with ageing. It was concluded by Prawitt et.al. [22] that the increased plasma bile acid levels could not explain the improved glucose control, since lowering of bile acids using colesevelam did not change glucose levels in Fxr deficient animals. However, they observed that the body weight gain was slightly increased by colesevelam, indicating that bile acids could take part in the reduced body weight gain in Fxr deficient mice [22]. It is therefore possible that increased plasma bile acid levels in older Fxr deficient mice are partly responsible for the reduced body weight gain and increased energy expenditure. Bile acids increase energy expenditure by activating the G-protein-coupled receptor TGR5 in brown adipose tissue and skeletal muscle [34]. It is therefore likely that the increased energy expenditure is at least partly explained by increased bile acid levels activating TGR5. Increased energy expenditure is a powerful way of enhancing glucose control via increased insulin sensitivity as exemplified by brown adipose tissue transplantation [35], increased energy expenditure in the context of increased inflammation [36] or a primary defect in the skin resulting in increased heat loss and energy expenditure [37]. The most plausible explanation to the improved glucose tolerance in the ageing Fxr deficient mice is therefore increased energy expenditure.
The ageing Fxr deficient mice did not gain body weight and had a markedly reduced percentage of body fat as compared to the WT mice. Since there were no significant differences in energy intake or fecal energy loss, the reduced body weight gain is most likely explained by the increased energy expenditure. There are several potential explanations to the increased energy expenditure in the Fxr deficient mice and some of these explanations were ruled out in this study. Fxr deficiency was not accompanied by increased locomotor activity or core body temperature and the unaltered body temperature together with the lower weight of the BAT depot argues against a primary effect in that tissue. However, we cannot rule out that TGR5 activation of energy production in BAT and skeletal muscle contributed to the increased energy production. Thus, increased energy expenditure that is not explained by increased locomotor activity or core body temperature could possibly be explained by increased heat loss via the skin. Although no major structural changes of the skin were observed on the Fxr deficient mice, it does not exclude that the increased energy expenditure in older Fxr deficient animals is explained by increased heat loss through superficial vasodilatation and activation of counter-current temperature systems in skin, nasal conchae and tail. Hypothetically, direct epidermal convection heat loss cannot be excluded, and would possibly be supported by the finding that FXR may be of importance for development of the fetal epidermal permeability barrier [38]. The increased weight of the liver observed in the present study in the Fxr deficient mice together with previous findings suggesting that PPARαactivation can contribute to increased energy expenditure [33] led us to investigate whether there are signs of increased PPARα activation in the liver from the Fxr deficient mice. Liver expression of Pparα was reduced but there were no changes in two down-stream target genes indicating no major change in Pparα signalling. We therefore believe it is unlikely that increased PPARα activation could have contributed to increased energy expenditure and liver weight. The increased liver weight was not explained by the increased liver triglyceride content since it increased from approximately 6% in WT controls to 9% of the total liver weight in the Fxr deficient mice. Increased liver triglycerides in Fxr deficient mice have been reported before [7], [24]. Increased flux of fatty acids to the liver because of reduced adipogenesis [7] as well as increased hepatic de novo lipogenesis has been suggested to explain increased liver triglyceride content in the Fxr deficient mice [4], [24], [39]. In the present study, we did not find evidence for either increased de novo lipogenesis or increased flux of fatty acids. It is therefore most likely that the small increase in liver triglycerides is a sign of hepatocyte dysfunction resulting in retention of lipids. In line with our findings, Fxr deficient mice at 15 months of age display increased liver size [16]. Increased liver expression of cyclin D1 and E1 of old Fxr deficient mice indicated that the cause of the increased liver size was increased cell division. Hence, the increased liver weight in the Fxr deficient mice is likely explained by hyperplasia.
The Fxr deficient mice suffered from cholestasis as indicated by yellowish discoloured liver, paws and plasma and very high plasma levels of bilirubin and bile acids. As expected from previous studies [5], [39], the expression of Cyp7a1 and Cyp8b1 were markedly increased in the Fxr deficient mice, most likely resulting in increased production of bile acids. Normal expression of Abcb11 (BSEP) is rate-limiting for pumping bile acids from the hepatocytes into the bile canaliculi. The expression of Abcb11 was markedly reduced in the Fxr deficient mice as shown before [39] and reduced function or expression of Abcb11 results in a clinical syndrome of intrahepatic cholestasis [40], [41]. Interestingly, hepatic overexpression of Abcb11 reduced hepatic lipids [42], indicating that the markedly reduced Abcb11 expression could contribute not only to cholestasis but also to the observed increase in liver triglycerides.
The old Fxr deficient mice in the current study displayed a picture of cholestasis and steatohepatitis despite improved glucose control and no dietary challenges. Very high plasma levels of bile acids, bilirubin, ALT and cholesterol indicated dysfunctional liver metabolism and hepatic damage in the Fxr deficient mice. The histological examination revealed high degree of perisinusoidal/sinusoidal foam cells, ballooning degeneration and lobular inflammation in the Fxr deficient animals. A similar pathology has been described to occur in livers of Fxr deficient mice on Ldlr deficient background, and more pronounced when fed HFD [24]. The liver of the old Fxr deficient mice had increased expression of Tnfα, HO-1, Ccl5, Tlr-4 and Cd11c. Increased expression of TNFα is a common feature of different models of NASH [43] and observed in other Fxr deficient models displaying liver injury [16], [17], [24]. Increased oxidative stress also seems to be a common feature of various models of NASH [43]. NASH patients have increased HO-1 expression and the increased expression is regarded as an adaptive response protecting against oxidative damage [44]. Marked induction of HO-1 expression following BACH1 deficiency protects from methionine-choline deficiency induced NASH [45]. Ccl5 mRNA expression was increased more than 2-fold. CCL5 is a chemokine with potent chemoattractant activity for T-lymphocytes and monocytes that have been shown to promote hepatic inflammation and fibrosis in a bile duct ligation model. Moreover, patients with cirrhosis show marked up-regulation of Ccl5 mRNA [46]. In line with increased Ccl5 expression, the expression of Cd11c was increased indicating increased myeloid cell activity or number.
A remaining question is what mechanisms could contribute to inflammatory changes resulting in steatohepatitis in ageing Fxr deficient mice. One possibility is indicated from studies of the antibacterial defence in the small intestine of Fxr deficient animals [47]. It was shown that Fxr deficient mice display increased levels of ileal bacteria and a reduced gut barrier function. In the current study, Fxr deficient mice displayed markedly increased weight of the ceacum, indicating changed gut microbiota. Thus, it is possible that increased amounts of bacterial products, e.g. endotoxins, might have contributed to the liver damage and inflammation observed in the ageing Fxr deficient mice. Indeed, Tlr-4 deficiency has been shown to protect from diet induced liver inflammation and injury [48] and the present results showing increased expression of the Tlr-4 receptor indicates increased susceptibility to a second hit involving endotoxins. Moreover, it has been suggested that FXR is important for liver repair by promoting regeneration and preventing cell death [17]. Hence, the effects observed in the present study of liver dysfunction may partly be explained by the lack of the liver repair functions of FXR in combination with the cholestasis.
An interesting observation in the present study is that ageing Fxr deficient mice had reduced bone mineral density and content. Few studies have investigated the importance of FXR for bone metabolism [49]. They found that FXR activation of human bone marrow stromal cells differentiate these cells into osteoblasts. In contrast, FXR inhibition resulted in an adipocytes-like phenotype [49]. Therefore, it is likely that the ageing Fxr deficient mice experience reduced bone mass because of reduced osteoblast differentiation and function.
In summary, this study extends previous observations about the importance of Fxr in metabolic regulation by studying single housed male mice of a novel Fxr deficient mouse line during ageing. The study sheds light on the long-term consequences of Fxr deficiency under normal dietary conditions on energy-, glucose and lipid metabolism. The most striking observation was the serious liver damage including cholestasis and steatohepatitis, resembling NASH, which occurred in the context of leanness and improved glucose homeostasis, strengthening the view that FXR is of major importance for normal liver functions. We conclude that FXR antagonism does not represent an attractive drug target.
Acknowledgments
We would like to acknowledge Marie Jönsson for performing animal experiments and Anders Elmgren, Charlotte Lindgren and Lena Amrot Fors for performing the blood plasma analyses. Also, we would like to acknowledge Meint Schuelke for bioinformatics support and Sandra Eng for expression level analyses.
Author Contributions
Conceived and designed the experiments: MB MW TA GB MG DL KB MB-Y. Performed the experiments: MB MW TA MH GB MG DL KB JO MB-Y. Analyzed the data: MB TA MH GB MG DL KB JO MB-Y. Contributed reagents/materials/analysis tools: MB MW TA MH GB MG. Wrote the paper: MB DL KB JO MB-Y.
References
- 1. Forman BM, Goode E, Chen J, Oro AE, Bradley DJ, et al. (1995) Identification of a nuclear receptor that is activated by farnesol metabolites. Cell 81: 687–693.
- 2. Parks DJ, Blanchard SG, Bledsoe RK, Chandra G, Consler TG, et al. (1999) Bile acids: Natural ligands for an orphan nuclear receptor. Science 284: 1365–1368.
- 3. Lambert G, Amar MJ, Guo G, Brewer HB Jr, Gonzalez FJ, et al. (2003) The farnesoid X-receptor is an essential regulator of cholesterol homeostasis. J Biol Chem 278: 2563–2570.
- 4. Ma K, Saha PK, Chan L, Moore DD (2006) Farnesoid X receptor is essential for normal glucose homeostasis. J Clin Invest 116: 1102–1109.
- 5. Sinal CJ, Tohkin M, Miyata M, Ward JM, Lambert G, et al. (2000) Targeted disruption of the nuclear receptor FXR/BAR impairs bile acid and lipid homeostasis. Cell 102: 731–744.
- 6. Zhang Y, Ge X, Heemstra LA, Chen WD, Xu J, et al. (2012) Loss of FXR protects against diet-induced obesity and accelerates liver carcinogenesis in ob/ob mice. Mol Endocrinol 26: 272–280.
- 7. Cariou B, van Harmelen K, Duran-Sandoval D, van Dijk TH, Grefhorst A, et al. (2006) The farnesoid X receptor modulates adiposity and peripheral insulin sensitivity in mice. J Biol Chem 281: 11039–11049.
- 8. Goodwin B, Jones SA, Price RR, Watson MA, McKee DD, et al. (2000) A regulatory cascade of the nuclear receptors FXR, SHP-1, and LRH-1 represses bile acid biosynthesis. Mol Cell 6: 517–526.
- 9. Kim I, Ahn SH, Inagaki T, Choi M, Ito S, et al. (2007) Differential regulation of bile acid homeostasis by the farnesoid X receptor in liver and intestine. J Lipid Res 48: 2664–2672.
- 10. Inagaki T, Choi M, Moschetta A, Peng L, Cummins CL, et al. (2005) Fibroblast growth factor 15 functions as an enterohepatic signal to regulate bile acid homeostasis. Cell Metab 2: 217–225.
- 11. Song KH, Li T, Owsley E, Strom S, Chiang JY (2009) Bile acids activate fibroblast growth factor 19 signaling in human hepatocytes to inhibit cholesterol 7alpha-hydroxylase gene expression. Hepatology 49: 297–305.
- 12. Kok T, Hulzebos CV, Wolters H, Havinga R, Agellon LB, et al. (2003) Enterohepatic circulation of bile salts in farnesoid X receptor-deficient mice: Efficient intestinal bile salt absorption in the absence of ileal bile acid-binding protein. J Biol Chem 278: 41930–41937.
- 13. van Dijk TH, Grefhorst A, Oosterveer MH, Bloks VW, Staels B, et al. (2009) An increased flux through the glucose 6-phosphate pool in enterocytes delays glucose absorption in fxr-/- mice. J Biol Chem 284: 10315–10323.
- 14. Zhang Y, Wang X, Vales C, Lee FY, Lee H, et al. (2006) FXR deficiency causes reduced atherosclerosis in ldlr-/- mice. Arterioscler Thromb Vasc Biol 26: 2316–2321.
- 15. Zhang Y, Lee FY, Barrera G, Lee H, Vales C, et al. (2006) Activation of the nuclear receptor FXR improves hyperglycemia and hyperlipidemia in diabetic mice. Proc Natl Acad Sci U S A 103: 1006–1011.
- 16. Yang F, Huang X, Yi T, Yen Y, Moore DD, et al. (2007) Spontaneous development of liver tumors in the absence of the bile acid receptor farnesoid X receptor. Cancer Res 67: 863–867.
- 17. Meng Z, Wang Y, Wang L, Jin W, Liu N, et al. (2010) FXR regulates liver repair after CCl4-induced toxic injury. Mol Endocrinol 24: 886–897.
- 18. Huang W, Ma K, Zhang J, Qatanani M, Cuvillier J, et al. (2006) Nuclear receptor-dependent bile acid signaling is required for normal liver regeneration. Science 312: 233–236.
- 19. Hashidume T, Sasaki T, Inoue J, Sato R (2011) Consumption of soy protein isolate reduces hepatic SREBP-1c and lipogenic gene expression in wild-type mice, but not in FXR-deficient mice. Biosci Biotechnol Biochem 75: 1702–1707.
- 20. Lian F, Xing X, Yuan G, Schafer C, Rauser S, et al. (2011) Farnesoid X receptor protects human and murine gastric epithelial cells against inflammation-induced damage. Biochem J 438: 315–323.
- 21. Dufer M, Horth K, Wagner R, Schittenhelm B, Prowald S, et al. (2012) Bile acids acutely stimulate insulin secretion of mouse beta-cells via farnesoid X receptor activation and K(ATP) channel inhibition. Diabetes 61: 1479–1489.
- 22. Prawitt J, Abdelkarim M, Stroeve JH, Popescu I, Duez H, et al. (2011) Farnesoid X receptor deficiency improves glucose homeostasis in mouse models of obesity. Diabetes 60: 1861–1871.
- 23. Wang XX, Jiang T, Shen Y, Caldas Y, Miyazaki-Anzai S, et al. (2010) Diabetic nephropathy is accelerated by farnesoid X receptor deficiency and inhibited by farnesoid X receptor activation in a type 1 diabetes model. Diabetes 59: 2916–2927.
- 24. Kong B, Luyendyk JP, Tawfik O, Guo GL (2009) Farnesoid X receptor deficiency induces nonalcoholic steatohepatitis in low-density lipoprotein receptor-knockout mice fed a high-fat diet. J Pharmacol Exp Ther 328: 116–122.
- 25. Maran RR, Thomas A, Roth M, Sheng Z, Esterly N, et al. (2009) Farnesoid X receptor deficiency in mice leads to increased intestinal epithelial cell proliferation and tumor development. J Pharmacol Exp Ther 328: 469–477.
- 26. Cariou B, van Harmelen K, Duran-Sandoval D, van Dijk T, Grefhorst A, et al. (2005) Transient impairment of the adaptive response to fasting in FXR-deficient mice. FEBS Lett 579: 4076–4080.
- 27. Soriano P (1999) Generalized lacZ expression with the ROSA26 cre reporter strain. Nat Genet 21: 70–71.
- 28. Gerdin AK, Surve VV, Jonsson M, Bjursell M, Bjorkman M, et al. (2006) Phenotypic screening of hepatocyte nuclear factor (HNF) 4-gamma receptor knockout mice. Biochemical & Biophysical Research Communications 349: 825–832.
- 29. Bjursell M, Ahnmark A, Bohlooly YM, William-Olsson L, Rhedin M, et al. (2007) Opposing effects of adiponectin receptors 1 and 2 on energy metabolism. Diabetes 56: 583–93.
- 30. Bjursell M, Admyre T, Goransson M, Marley AE, Smith DM, et al. (2011) Improved glucose control and reduced body fat mass in free fatty acid receptor 2-deficient mice fed a high-fat diet. Am J Physiol Endocrinol Metab 300: E211–20.
- 31. Bjursell M, Egecioglu E, Gerdin AK, Svensson L, Oscarsson J, et al. (2005) Importance of melanin-concentrating hormone receptor for the acute effects of ghrelin. Biochemical & Biophysical Research Communications 326: 759–765.
- 32. Edvardsson U, Ljungberg A, Linden D, William-Olsson L, Peilot-Sjogren H, et al. (2006) PPARalpha activation increases triglyceride mass and adipose differentiation-related protein in hepatocytes. J Lipid Res 47: 329–340.
- 33. Srivastava RA, Jahagirdar R, Azhar S, Sharma S, Bisgaier CL (2006) Peroxisome proliferator-activated receptor-alpha selective ligand reduces adiposity, improves insulin sensitivity and inhibits atherosclerosis in LDL receptor-deficient mice. Mol Cell Biochem 285: 35–50.
- 34. Watanabe M, Houten SM, Mataki C, Christoffolete MA, Kim BW, et al. (2006) Bile acids induce energy expenditure by promoting intracellular thyroid hormone activation. Nature 439: 484–489.
- 35. Gunawardana SC, Piston DW (2012) Reversal of type 1 diabetes in mice by brown adipose tissue transplant. Diabetes 61: 674–682.
- 36. Tang T, Zhang J, Yin J, Staszkiewicz J, Gawronska-Kozak B, et al. (2010) Uncoupling of inflammation and insulin resistance by NF-kappaB in transgenic mice through elevated energy expenditure. J Biol Chem 285: 4637–4644.
- 37. Binczek E, Jenke B, Holz B, Gunter RH, Thevis M, et al. (2007) Obesity resistance of the stearoyl-CoA desaturase-deficient (scd1-/-) mouse results from disruption of the epidermal lipid barrier and adaptive thermoregulation. Biol Chem 388: 405–418.
- 38. Hanley K, Jiang Y, Crumrine D, Bass NM, Appel R, et al. (1997) Activators of the nuclear hormone receptors PPARalpha and FXR accelerate the development of the fetal epidermal permeability barrier. J Clin Invest 100: 705–712.
- 39. Moschetta A, Bookout AL, Mangelsdorf DJ (2004) Prevention of cholesterol gallstone disease by FXR agonists in a mouse model. Nat Med 10: 1352–1358.
- 40. Chen F, Ananthanarayanan M, Emre S, Neimark E, Bull LN, et al. (2004) Progressive familial intrahepatic cholestasis, type 1, is associated with decreased farnesoid X receptor activity. Gastroenterology 126: 756–764.
- 41. Strautnieks SS, Bull LN, Knisely AS, Kocoshis SA, Dahl N, et al. (1998) A gene encoding a liver-specific ABC transporter is mutated in progressive familial intrahepatic cholestasis. Nat Genet 20: 233–238.
- 42. Figge A, Lammert F, Paigen B, Henkel A, Matern S, et al. (2004) Hepatic overexpression of murine Abcb11 increases hepatobiliary lipid secretion and reduces hepatic steatosis. J Biol Chem 279: 2790–2799.
- 43. Takahashi Y, Soejima Y, Fukusato T (2012) Animal models of nonalcoholic fatty liver disease/nonalcoholic steatohepatitis. World J Gastroenterol 18: 2300–2308.
- 44. Malaguarnera L, Madeddu R, Palio E, Arena N, Malaguarnera M (2005) Heme oxygenase-1 levels and oxidative stress-related parameters in non-alcoholic fatty liver disease patients. J Hepatol 42: 585–591.
- 45. Inoue M, Tazuma S, Kanno K, Hyogo H, Igarashi K, et al. (2011) Bach1 gene ablation reduces steatohepatitis in mouse MCD diet model. J Clin Biochem Nutr 48: 161–166.
- 46. Seki E, De Minicis S, Gwak GY, Kluwe J, Inokuchi S, et al. (2009) CCR1 and CCR5 promote hepatic fibrosis in mice. J Clin Invest 119: 1858–1870.
- 47. Inagaki T, Moschetta A, Lee YK, Peng L, Zhao G, et al. (2006) Regulation of antibacterial defense in the small intestine by the nuclear bile acid receptor. Proc Natl Acad Sci U S A 103: 3920–3925.
- 48. Ye D, Li FY, Lam KS, Li H, Jia W, et al. (2012) Toll-like receptor-4 mediates obesity-induced non-alcoholic steatohepatitis through activation of X-box binding protein-1 in mice. Gut 61: 1058–1067.
- 49. Id Boufker H, Lagneaux L, Fayyad-Kazan H, Badran B, Najar M, et al. (2011) Role of farnesoid X receptor (FXR) in the process of differentiation of bone marrow stromal cells into osteoblasts. Bone 49: 1219–1231.