Regulation of plasma triglyceride partitioning by adipose-derived ANGPTL4 in mice

Spitler, Kathryn M.; Shetty, Shwetha K.; Cushing, Emily M.; Sylvers-Davie, Kelli L.; Davies, Brandon S. J.

doi:10.1038/s41598-021-87020-5

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Published: 12 April 2021

Regulation of plasma triglyceride partitioning by adipose-derived ANGPTL4 in mice

Kathryn M. Spitler¹,
Shwetha K. Shetty¹,
Emily M. Cushing¹,
Kelli L. Sylvers-Davie¹ &
…
Brandon S. J. Davies¹

Scientific Reports volume 11, Article number: 7873 (2021) Cite this article

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Abstract

Elevated plasma triglyceride levels are associated with metabolic disease. Angiopoietin-like protein 4 (ANGPTL4) regulates plasma triglyceride levels by inhibiting lipoprotein lipase (LPL). Our aim was to investigate the role of adipocyte-specific deficiency of ANGPTL4 in mice during high fat diet feeding. Adipocyte-specific ANGPTL4 deficient mice were fed a high fat diet (60% kCal from fat) for either 12 weeks or 6 months. We performed plasma metabolic measurements, triglyceride clearance and uptake assays, LPL activity assays, and assessed glucose homeostasis. Mice lacking adipocyte ANGPTL4 recapitulated the triglyceride phenotypes of whole-body ANGPTL4 deficiency, including increased adipose LPL activity, lower plasma triglyceride levels, and increased uptake of triglycerides into adipose tissue. When fed a high fat diet (HFD), these mice continued to display enhanced adipose LPL activity and initially had improved glucose and insulin sensitivity. However, after 6 months on HFD, the improvements in glucose homeostasis were largely lost. Moreover, despite higher adipose LPL activity levels, mice lacking adipocyte ANGPTL4 no longer had increased triglyceride uptake into adipose compared to littermate controls after chronic high-fat feeding. These observations suggest that after chronic high-fat feeding LPL is no longer rate-limiting for triglyceride delivery to adipocytes. We conclude that while adipocyte-derived ANGPTL4 is an important regulator of plasma triglyceride levels and triglyceride partitioning under normal diet conditions, its role is diminished after chronic high-fat feeding.

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Introduction

Elevated plasma triglyceride levels have been implicated in the pathology of a variety of cardiovascular and metabolic diseases. Circulating triglycerides are hydrolyzed by lipoprotein lipase (LPL), releasing fatty acids that are taken up and utilized by tissues. Angiopoietin-like protein 4 (ANGPTL4), a secreted factor induced by fasting and expressed in several metabolically active tissues, inhibits LPL activity and thereby regulates plasma triglyceride levels^1,2,3,4,5. Genetic loss of ANGPTL4 leads to decreased fasting plasma triglyceride levels in both humans and mice, and humans deficient in ANGPTL4 appear to be protected from cardiovascular disease^6,7,8. Moreover, a recent study found that human carriers of the common ANGPTL4 inactivating mutant E40K were protected against obesity-associated dyslipidemia⁹. However, whether these protections are conferred by loss of ANGPTL4 in a specific tissue or require systemic loss of ANGPTL4 remains unclear.

ANGPTL4 is expressed highly in adipose depots³. In the last twenty years the work of many labs has led to development of a model where, during fasting, adipose-derived ANGPTL4 is rapidly induced and acts locally to inhibit adipose LPL activity and triglyceride uptake, diverting triglycerides to other tissues^3,5,10,11,12. Recent studies using Angptl4^–/– or adipose-specific Angptl4 knockout mice strongly support this model by showing that fasted mice lacking ANGPTL4 have increased uptake of triglycerides specifically in adipose tissue^13,14. The role of ANGPTL4 in mediating or alleviating metabolic disturbances induced by high-fat feeding has not been fully studied. Such studies have been hindered by the fact that Angptl4^–/– mice fed a high fat diet (HFD) develop a lethal intestinal injury and lymphatic nodule inflammation¹⁵.

In this study, we sought to define the adipose-specific actions of ANGPTL4 more clearly. To this end, we generated adipocyte-specific Angptl4 knockout mice and studied their triglyceride and metabolic phenotypes when fed normal chow and high-fat diets. The effects of adipocyte-specific ANGPTL4-deficiency on triglyceride and glucose homeostasis were determined after 12 weeks of high-fat feeding, as well as after 6 months of high-fat feeding to model a chronic state of obesity.

Results

Effects of adipocyte-specific ANGPTL4 deficiency on plasma TG levels and TG uptake into tissues

To examine the adipose-specific role of ANGPTL4, we generated adipocyte-specific Angptl4 knockout mice. To do so, we first generated Angptl4-floxed mice (Angptl4^fl/fl) by utilizing CRISPR/Cas9 to insert LoxP sites in the introns between exons 1 and 2 and between exons 3 and 4 (Supplemental Fig. 1a). Recombination between LoxP sites generates a frame-shift resulting in a truncated (145 aa) protein in which the final 35 amino acids do not match the native sequence. Adipocyte-specific (Angptl4^AdipoKO) mice were generated by crossing Angptl4^fl/fl mice with mice expressing the adiponectin-Cre. To assess the impact of Cre-mediated recombination on Angptl4 expression, we performed qPCR with 7 different primer sets on brown adipose tissue (BAT) from Angptl4^AdipoKO mice (Supplemental Fig. 1b). Compared to Cre negative controls, significantly reduced expression was observed with all 7 primer sets (Supplemental Fig. 1c). qPCR signal was further reduced when using primer sets targeting exons 2 and 3, the exons removed by recombination (Supplemental Fig. 1c). Together these data implied that Cre-mediated recombination was successful and that the recombined gene resulted in greatly reduced RNA expression of Angptl4.

Ideally, levels of ANGPTL4 protein would be assessed to ensure knockout of ANGPTL4, however no currently available antibodies are specific for mouse ANGPTL4. To assess if our recombined allele would still make protein, we generated a plasmid construct mimicking the predicted protein product of our Angptl4 flox allele after Cre-mediated recombination. We also generated a plasmid construct mimicking the post-recombination protein product of the Angptl4 flox allele generated by the KOMP mouse repository and used in other studies of the tissue-specific actions of ANGPTL4^13,16,17. 293 T cells were transfected with these constructs or a construct expressing full-length wildtype mouse ANGPTL4 and both cell lysate and the media were subjected to Western blot analysis. As expected, in cells transfected with the full-length construct, we observed ANGPTL4 protein in both the cell lysate and secreted in the media (Supplemental Fig. 1d). We observed no protein expression in either the lysate or the media from the construct representing our flox allele, suggesting that after Cre recombination our flox allele does not produce protein. Interestingly, we did observe substantial protein expression in the lysate from the construct representing the KOMP allele, though very little of this protein appeared to be secreted (Supplemental Fig. 1d). When the conditioned media from these constructs were tested for their ability to inhibit LPL, neither the media from our allele, nor the media containing the small amount of secreted protein from the KOMP flox allele were able to inhibit LPL activity (Supplemental Fig. 1e).

We examined Angptl4 expression in metabolically active tissues in our adipocyte-specific Angptl4–deficient mice. As expected, expression of Angptl4 in gonadal, subcutaneous, and brown adipose tissues (gWAT, sWAT, BAT) was significantly reduced in Angptl4^AdipoKO mice, while being preserved in other tissues (Fig. 1a). Fasting plasma triglyceride levels were significantly lower in 8-week–old male and female Angptl4^AdipoKO mice compared to Angptl4^fl/fl mice (Fig. 1b). These results suggest that the lower plasma TG levels observed in Angptl4 whole-body knockout mice^2,14,18 is due to the loss of adipocyte-derived ANGPTL4. We observed a decrease in fasting plasma free fatty acid levels in male, but not female Angptl4^AdipoKO mice compared to Angptl4^fl/fl mice (Fig. 1c). There were no genotype-specific differences in fasting blood glucose levels between groups (Fig. 1d).

We previously observed increased plasma triglyceride clearance, increased adipose uptake of triglycerides, and increased adipose LPL activity in whole-body Angptl4^–/– mice¹⁴. In that study we inferred that the increased clearance was due to ANGPTL4 deficiency specifically in the adipose tissue¹⁴. To determine if this was indeed the case, we performed triglyceride clearance assays on female Angptl4^AdipoKO mice using radiolabeled chylomicrons. We also assessed uptake of radiolabeled chylomicrons into specific tissues. After an intravenous injection of radiolabeled chylomicrons, Angptl4^AdipoKO mice cleared the radiolabeled TGs from the plasma faster than Angptl4^fl/fl mice (Fig. 1e). Similar to what we had observed with whole-body Angptl4^–/– mice¹⁴, Angptl4^AdipoKO female mice had increased radiolabel uptake into adipose depots compared to Angptl4^fl/fl mice (Fig. 1f). As with whole-body Angptl4^–/– mice, LPL activity was increased in white adipose tissue of female Angptl4^AdipoKO mice compared to Angptl4^fl/fl mice (Fig. 1g,h). Additionally, there was a decrease in LPL activity in heart tissue of female Angptl4^AdipoKO mice compared to Angptl4^fl/fl mice. These data support our previous supposition that deficiency in adipose ANGPTL4 is responsible for the increased triglyceride uptake into adipose tissue.

Effects of high-fat feeding on body phenotypes and plasma parameters in adipocyte-specific ANGPTL4–deficient mice

Given the importance of ANGPTL4 in directing triglycerides away from adipose tissue¹⁴, we sought to determine how high-fat feeding would alter metabolic phenotypes in Angptl4^AdipoKO and Angptl4^fl/fl mice. We randomly assigned Angptl4^AdipoKO and Angptl4^fl/fl mice at 8 weeks of age to a normal chow (NCD) or high fat diet (HFD; 60% kCal/fat) and fed them the respective diet for 12 weeks. On HFD, body weight gain was similar between all groups (Fig. 2a). No genotype-specific differences in tissue weights were observed (Fig. 2b). Adiposity, as determined by NMR, was greater in all mice fed a HFD compared to mice fed a NCD (Fig. 2c). Despite no differences in body weight, some Angptl4^AdipoKO mice on NCD had significantly more total fat mass compared to Angptl4^fl/fl mice (Fig. 2c). This genotype-specific difference in fat mass was not seen in HFD-fed Angptl4^AdipoKO mice (Fig. 2c).

As before, Angptl4^AdipoKO mice had lower fasting plasma TG levels compared to Angptl4^fl/fl mice (Fig. 2d). Neither HFD nor adipocyte ANGPTL4 deficiency altered plasma non-esterified fatty acid levels (Fig. 2e). HFD feeding for 12 weeks increased plasma glucose and liver triglyceride levels in all groups, and the increase in liver triglycerides was higher in Angptl4^AdipoKO mice than that in Angptl4^fl/fl mice. (Fig. 2f,g).

Tissue expression of Angptl4 was influenced both by genotype and by diet. As expected, expression of Angptl4 in gonadal, subcutaneous, and brown adipose tissues (eWAT, sWAT, BAT) was much lower in Angptl4^AdipoKO mice compared to Angptl4^fl/fl mice (Supplemental Fig. 2a). Surprisingly, Angptl4^AdipoKO mice on NCD had greatly reduced Angptl4 expression in the heart compared to Angptl4^fl/fl mice (Supplemental Fig. 2a), suggesting that loss of ANGPTL4 in the adipose tissue had a systemic effect leading to downregulation of ANGPTL4 in other tissues. Interestingly, HFD alone significantly decreased Angptl4 expression in several tissues, including the heart, liver, and white adipose tissue (Supplemental Fig. 2a). These data indicate that high fat feeding can regulate expression of Angptl4. We also measured tissue gene expression of Lpl and found no genotype-specific differences (Supplemental Fig. 2b).

As changes in energy expenditure play a role in the pathogenesis of obesity, we asked if adipocyte-specific loss of ANGPTL4 would lead to changes in energy expenditure, oxygen consumption (VO₂), carbon dioxide production (VCO₂), or respiratory quotient (RQ; VCO₂/VO₂). Using the Promethion metabolic caging system, we observed no differences in energy expenditure, VO₂, VCO₂, or RQ in Angptl4^AdipoKO mice on either a NCD or HFD compared to Angptl4^fl/fl mice (Supplemental Fig. 3).

Effects of high-fat feeding on TG uptake and LPL activity in adipocyte-specific ANGPTL4 deficient mice

To assess if high-fat diet feeding altered triglyceride partitioning in an ANGPTL4-dependent manner, we performed plasma triglyceride clearance and tissue uptake assays on male Angptl4^AdipoKO mice at the end of 12 weeks of either NCD or HFD feeding. On a NCD, Angptl4^AdipoKO mice cleared radiolabeled TGs from the plasma faster than Angptl4^fl/fl mice (Fig. 3a). Mice fed a HFD had faster clearance of plasma triglycerides than those fed a NCD, but on HFD there were no genotype-specific differences in clearance rates (Fig. 3a). Consistent with our observations in female mice, on NCD Angptl4^AdipoKO male mice had increased radiolabel uptake into epididymal and subcutaneous adipose depots compared to floxed controls (Fig. 3b). Interestingly, on HFD, the differences in radiolabel uptake into adipose tissues between Angptl4^AdipoKO mice and Angptl4^fl/fl littermates were reduced (Fig. 3b). These data again support the idea that on a NCD, deficiency in adipose ANGPTL4 results in increased triglyceride uptake into adipose tissue, but also suggest that this difference decreases in the face of high-fat feeding.

To elucidate if the increased uptake of triglyceride-derived fatty acids into adipose tissue in Angptl4^AdipoKO mice was the result of increased LPL activity we measured tissue lipase activity. LPL activity was greater in the gonadal adipose tissue of Angptl4^AdipoKO mice on both NCD or HFD compared to Angptl4^fl/fl mice (Fig. 3c). HFD itself altered LPL activity in some tissues, increasing activity in quadricep muscle and slightly decreasing activity in epididymal white adipose tissue (Fig. 3c). We also assessed if loss of ANGPTL4 resulted in changes in liver lipase activity. As expected, LPL activity in the liver was low compared to total lipase activity. We found no genotype-specific differences in total lipase, hepatic lipase, or LPL activity on either diet in the Angptl4^AdipoKO mice compared to Angptl4^fl/fl mice (Fig. 3d,e). Together, TG clearance and LPL activity in Angptl4^AdipoKO mice closely resemble those we have previously reported in whole-body ANGPTL4 knockout mice¹⁴, supporting the idea that the lack of adipose-derived ANGPTL4 is the primary driver of the increased adipose LPL activity and TG clearance in those mice.

Effects of high-fat feeding on glucose tolerance and insulin sensitivity in adipocyte-specific ANGPTL4–deficient mice

A previous report found that an independent strain of adipocyte-specific ANGPTL4 knockout mice had improved glucose tolerance compared to wild-type mice after being fed a HFD for 4 weeks¹³. To assess if the loss of adipocyte-derived ANGPTL4 altered glucose metabolism in our mice, we performed glucose (GTT) and insulin tolerance (ITT) tests. On a normal chow diet, no differences were observed in glucose tolerance or insulin sensitivity in Angptl4^AdipoKO mice compared to floxed controls (Fig. 4). However, glucose tolerance and insulin sensitivity were markedly improved in HFD-fed Angptl4^AdipoKO mice compared to HFD-fed floxed controls (Fig. 4a,b). These data support a protective role for loss of adipose-derived ANGPTL4 on systemic glucose homeostasis. Chronic inflammation has been linked with insulin resistance during obesity and type 2 diabetes¹⁹. To test whether the changes we observed in glucose tolerance and insulin sensitivity were due to changes in tissue inflammation we measured tissue expression (liver, eWAT, sWAT, and BAT) of inflammatory markers C–C Motif Chemokine Ligand 2 (Ccl2), Cd68, and tumor necrosis factor α (Tnfα). As expected, there was an increase in inflammation in all tested tissues of HFD-fed mice. However, no major genotype-specific differences were observed (Supplemental Fig. 4).

Effects of adipocyte-specific ANGPTL4 deficiency in mice after a chronic high-fat diet

To better characterize the role of ANGPTL4 in the setting of chronic obesity, we fed Angptl4^AdipoKO, and Angptl4^fl/fl mice a NCD or HFD (60% kCal/fat) for 6 months. Initially, there were no genotype-specific differences in weight gain between any of the diet groups (Fig. 5a). However, after 18 weeks on diet, the body weight curves began to diverge, with Angptl4^AdipoKO mice gaining modestly more weight than littermate Angptl4^fl/fl mice on both a NCD or and a HFD (Fig. 5a). There were no genotype-specific differences in tissue weights (Fig. 5b). Adiposity, as determined by NMR, was greater in all mice fed a HFD compared to mice fed a NCD, and there was a significant increase in total fat mass in the high fat fed Angptl4^AdipoKO mice compared to high fat fed Angptl4^fl/fl controls (Fig. 5c). After 6 months on diet, Angptl4^AdipoKO mice continued to have significantly lower fasting plasma triglyceride levels compared to Angptl4^fl/fl mice (Fig. 5d). At this age, mice with ANGPTL4-deficiency in adipocytes tended to have lower plasma non-esterified fatty acids, but there were no genotype-specific differences in blood glucose or liver triglycerides levels (Fig. 5e–g). Interestingly, at this time point, the diet induced differences in blood glucose had disappeared and the diet-induced differences in liver TG had decreased (Fig. 5f,g).

As expected, expression of Angptl4 in the gonadal, subcutaneous and brown adipose tissues (eWAT, sWAT, BAT) of Angptl4^AdipoKO mice was much lower than in Angptl4^fl/fl littermates (Supplemental Fig. 5a). Similar to what we observed after 12 weeks on diet, expression of Angptl4 was reduced in Angptl4^AdipoKO mice in the heart and quadricep muscle compared to Angptl4^fl/fl. Also similar to what we observed after 12 weeks of high-fat feeding, Angptl4 expression was reduced in heart, liver, and white adipose tissue of Angptl4^fl/fl mice fed a HFD for 6 months, again supporting the idea that Angptl4 expression in these tissues is regulated by diet (Supplemental Fig. 5a). We also measured tissue gene expression of Lpl and found no genotype-specific differences (Supplemental Fig. 5b). As we consistently observed lower Angptl4 expression in the hearts of NCD-fed Angptl4^AdipoKO mice, we asked if this reduction was due to off-target cre recombination in the heart. To test this idea, we assessed recombination of the Angptl4 flox allele by performing PCR on genomic DNA isolated from the heart, eWAT, sWAT and BAT of Angptl4^AdipoKOand Angptl4^fl/fl mice fed a NCD for 6 months (Supplemental Fig. 5c). Angptl4 genomic recombination was seen in the fat pads of the Angptl4^AdipoKO mice but not Angptl4^fl/fl mice. Furthermore, no recombination was observed in the hearts of either genotype (Supplemental Fig. 5c), supporting the idea that the reduced expression of Angptl4 in heart was the result of some kind of feedback regulation.

To assess liver health in our mice we measured plasma activity of alanine aminotransferase (ALT) and aspartate aminotransferase (AST). All mice fed a HFD for 6 months had elevated AST and ALT activity compared to NCD fed mice, but no genotype-specific differences were observed (Supplemental Fig. 6a,b). We also measured inflammatory protein amyloid A in the plasma of our mice. Although HFD-fed mice had an increase in plasma amyloid A there were no genotype-specific differences (Supplemental Fig. 6c). Livers of mice fed a HFD were larger than those from mice fed NCD, but again no genotype-specific differences were observed (Supplemental Fig. 6d).

After 6 months on diet, Angptl4^AdipoKO mice continued to clear radiolabeled triglycerides from the plasma faster than littermate Angptl4^fl/fl mice on NCD (Fig. 6a). Angptl4^AdipoKO mice also cleared triglycerides faster when fed a HFD, though the difference was less pronounced (Fig. 6a). Again, Angptl4^AdipoKO male mice fed a NCD had increased uptake of radiolabeled fat into white adipose depots compared to floxed controls, but on HFD those differences largely disappeared (Fig. 6b). This was true even when we corrected for the somewhat faster plasma TG clearance in Angptl4^AdipoKO mice (Supplemental Fig. 7). To understand why adipose tissue ANGPTL4 deficiency no longer resulted in improved adipose clearance of triglycerides after a 6-month high-fat diet, we next measured tissue-specific LPL activity. After 6 months of high-fat feeding, LPL activity was still greater in the adipose depots of Angptl4^AdipoKO mice compared to those of Angptl4^fl/fl mice (Fig. 6c). These data suggest that during the setting of chronic high-fat feeding, increased LPL activity in the adipose tissue of Angptl4^AdipoKO mice no longer leads to increased adipose triglyceride uptake. We hypothesized that this could be that after chronic high feeding, LPL activity is no longer rate-limiting for triglyceride uptake. To assess if a chronic high-fat diet reduces expression of proteins involved in fatty acid uptake we measured the gene expression of Cd36, fatty acid transporters Fatp1 and Fapt4, and Acyl-CoA Synthetase Long Chain family members Acsl1 and Acsl4 in adipose tissues (Supplemental Fig. 8). Although we did observe a small decrease in Cd36 and Fatp1 expression in eWAT and decrease in Fatp1 expression in BAT following chronic high-fat feeding, we also observed increases in Cd36, Fatp4, and Acsl4 in sWAT, and Cd36 and Acsl1 in BAT (Supplemental Fig. 8). Thus, there was no clear indication that fatty acid uptake was downregulated at the gene expression level. Similar to what was observed after 12 weeks on HFD, there were no genotype-specific differences in total lipase, hepatic lipase, or LPL activity in the livers of Angptl4^AdipoKO mice after chronic high-fat diet feeding (Fig. 6d,e).

Finally, we asked if the disappearance of increased adipose triglyceride clearance after 6 months on HFD affected the improved glucose tolerance we had observed in Angptl4^AdipoKO mice after 12 weeks on HFD (see Fig. 6). Indeed, we found that Angptl4^AdipoKO mice no longer had improved glucose tolerance after 6 months on HFD (Fig. 7a). And while Angptl4^AdipoKO mice remained more insulin sensitive than Angptl4^fl/fl mice after 6 months on HFD, the improvement was greatly reduced compared to that observed after 12 weeks of HFD (Fig. 7b). As before, we measured tissue expression (liver, eWAT, sWAT, and BAT) of inflammatory markers Ccl2, Cd68 and Tnfα. Once again, there was an increase in inflammation in HFD-fed mice in tested tissues, but no major genotype-specific differences were observed (Supplemental Fig. 9).

Discussion

Proteins made and secreted by the adipose tissues play a vital role in lipid and glucose homeostasis during obesity. ANGPTL4 is highly expressed by adipose tissues in mice and humans^3,20,21,22. In this study we investigated the triglyceride phenotypes of adipocyte-specific ANGPTL4 knockout mice. We also investigated how adipocyte-specific loss of ANGPTL4 affected body weight, glucose tolerance, and insulin resistance in the setting of either 3 or 6 months of high-fat diet feeding and obesity. We found that adipocyte-specific loss of ANGPTL4 resulted in lower plasma triglycerides and increased uptake of triglyceride-fatty acids into adipose tissue when mice were fed a normal chow diet. When mice were fed a high-fat diet, we found that adipocyte-specific ANGPTL4 deletion initially resulted in improved glucose tolerance and insulin sensitivity, but over time this improvement disappeared, as did the increased adipose triglyceride uptake observed in normal chow fed mice.

The role of ANGPTL4 in regulating triglyceride metabolism through LPL inhibition has been well established. Human carriers of the E40K mutation in ANGPTL4 have lower triglycerides and a lower risk of coronary artery disease⁶ and dyslipidemia during obesity⁹. In mice, genetic loss of ANGPTL4 leads to decreased fasting plasma TG levels and increased uptake of triglycerides into adipose tissue^3,13,14,18. The specific increase in adipose tissue LPL activity and TG uptake in whole body ANGPTL4 knockout mice strongly supported the idea that adipose derived ANGPTL4 was responsible for the triglyceride phenotypes in whole-body ANGPTL4 knockout mice. Here, adipocyte-specific loss of ANGPTL4 in mice fed a chow diet phenocopies the triglyceride phenotypes observed in whole-body Angptl4^–/– mice. Angptl4^AdipoKO mice had lower plasma triglyceride levels, increased uptake of triglycerides into adipose tissue, and increased adipose tissue LPL activity. This was true in both male and female mice. The triglyceride phenotypes observed in Angptl4^AdipoKO mice were consistent with those recently reported by Aryal et al. using an independently derived adipocyte-specific ANGPTL4 knockout mouse¹³. Both studies support the hypothesis that it is primarily loss of adipose-derived ANGPTL4 that is responsible for the alterations in plasma triglyceride levels and triglyceride partitioning observed in Angptl4^–/– mice.

Angptl4^–/– mice fed a high-fat diet with high levels of saturated fat develop a lethal intestinal injury and lymphatic nodule inflammation¹⁵. In these mice serum amyloid A levels are extremely elevated after 8 weeks on diet (compared to wild-type mice) and Angptl4^–/– mice die after 15 to 25 weeks on diet¹⁵. Lethality on a high-fat diet was also observed in mice given an anti-ANGPTL4 antibody¹⁶. This phenotype appears to be mediated by the lack of macrophage ANGPTL4, allowing excessive lipid uptake into lymphatic macrophages¹⁵. In our study, we used adipose-specific ANGPTL4 conditional knockout mice in hopes of circumventing the high-fat feeding intestinal pathophysiology observed in whole-body knockout mice. As we did not observe increased serum amyloid A levels, increased hepatic inflammation, or increased mortality in HFD-fed Angptl4^AdipoKO mice compared to Angptl4^fl/fl mice, we conclude that adipose ANGPTL4 is not the primary protector against the lethal phenotype observed in HFD-fed Angptl4^–/– mice.

Loss of adipocyte ANGPTL4 in the context of HFD had an interesting effect on LPL activity and adipose triglyceride uptake. On a chow diet, the increase in adipose LPL activity in Angptl4^AdipoKO mice led to a corresponding increase in adipose tissue uptake of triglycerides. This connection between increased LPL activity and increased triglyceride uptake in adipose tissue was lost in mice fed a HFD. Adipose tissue LPL activity remained higher in Angptl4^AdipoKO mice fed a HFD compared to floxed control mice, but the enhanced adipose tissue uptake observed on chow diet was largely lost. These data suggest that on a chronic high-fat diet, LPL activity is no longer rate-limiting for the entry of triglyceride-derived fatty acids into adipose tissues. Why this would be the case is not clear. One possibility is that LPL-mediated lipolysis continues to occur, but uptake of these fatty acids into tissues is now limiting. The mechanisms by which fatty acids released by vascular lipolysis traverse capillary endothelial cells and are then taken up by adipocytes are not well understood. We measured gene expression of several genes associated with fatty acid uptake, but did not observe changes in expression that would clearly indicate a reduction in fatty acid uptake. However, our analysis did not encompass all genes associated with uptake, nor does gene expression necessarily corelate with functionality. Moreover, in our analysis we did not differentially analyze cell types within adipose tissues. A dramatic change in fatty acid uptake genes in endothelial cells might be masked by the lack of change or even increase in these same genes in adipocytes. Further, more targeted research will be needed to understand how fatty acid uptake is altered by long term high fat feeding and whether this may contribute to adipose dysfunction. Alternatively, it could be that changes in fatty acid uptake pathways are not responsible for the similar uptake in Angptl4^fl/fl and Angptl4^AdipoKO mice. It is possible that in Angptl4^AdipoKO mice other tissues uptake sufficient TGs to reduce the supply available to white adipose tissue. Although we did not see evidence of this in our uptake assays, it is important to note that we did not measure uptake in all tissues. The fact that Angptl4^AdipoKO mice fed a chronic HFD cleared plasma TGs somewhat faster and had lower plasma TG levels than Angptl4^fl/fl mice on the same diet suggest that there may indeed be tissues in Angptl4^AdipoKO mice that take up more TGs.

High-fat feeding experiments performed by Janssen et al.²³ suggested that ANGPTL4 deficiency not only impacts triglyceride metabolism, but also glucose metabolism. Their work demonstrated that Angptl4^–/– mice fed a diet rich in unsaturated fatty acids, gained more weight than wildtype mice, but had lower blood glucose levels and improved glucose tolerance. Indeed, human studies found that carriers of the inactivating E40K mutation in Angptl4 had lower fasting glucose levels than non-diabetic participants and had a lower odds ratio (0.89) for developing type 2 diabetes²⁴. One hypothesis is that improved glucose homeostasis is due to relief of LPL inhibition and improved triglyceride clearance to adipose tissues²³. Indeed, Aryal et al. found that after 4 weeks on HFD, adipose-specific Angptl4 knockout mice had improved glucose tolerance and insulin sensitivity¹³. We likewise found that Angptl4^AdipoKO mice had increased clearance of triglycerides to adipose tissues, and that after 12 weeks on HFD these mice have improved glucose tolerance and are protected from insulin resistance compared to control mice. However, in both our study and the Aryal study, the improved glucose tolerance and protection from insulin resistance were mostly lost after long-term HFD feeding. As discussed above, we found that chronically HFD fed Angptl4^AdipoKO mice did not have increased uptake of triglycerides into adipose tissue. We suspect that increasing TG partitioning to adipose tissues improves glucose homeostasis, but that when the increased TG uptake to adipose tissues is lost, improved glucose tolerance is also lost. Therapeutically, these findings imply that targeting ANGPTL4 to improve glucose tolerance may not be effective over the long-term, at least not in the situation of continued overconsumption of calories.

The current study is not without limitations. We chose a 60% (kCal) high fat diet, a diet that is widely used experimentally to induce an obese and insulin resistant phenotype. Other diets may more closely reflect the typical American diet, such as the “Western diet” comprised of 42% (kCal) high fat, high sucrose and high cholesterol. Alternative diets that induce different pathological states might illuminate tissue-specific roles for ANGPTL4 that were missed in our study. Another limitation to our study is that we studied adipocyte-specific Angptl4 knockout, but Angptl4 is expressed in other metabolically active tissues such as the liver. Therefore, we could have missed any synergistic effects of ANGPTL4 derived from adipose tissues with ANGPTL4 derived from other tissues. ANGPTL4 is expressed in liver^1,3,25, where its function is unknown. It is also expressed, although at lower levels, in skeletal muscle and heart²⁶ and could have important actions during exercise²⁷ or situations of lipotoxicity²⁸. ANGPTL4 expressed in the intestine has also been implicated in the effects of the intestinal microbiota on metabolism²³. Generating additional tissue-specific Angptl4 knockout mice could identify the roles of ANGPTL4 in these and other tissues.

Our studies highlight the importance of studying age and diet duration going forward. HFD studies in mice are generally performed in mice that are less than 1 year old and who have been fed a high-fat diet for 4 to 16 weeks. However, both Aryal et al.¹³ and our current study clearly showed that improved glucose tolerance in adipocyte-specific ANGPTL4 knockout mice disappeared with chronic high-fat feeding. Given that metabolic disease is most prevalent in older and obese populations, these observations highlight the need and importance of performing long-term feeding studies in aged mice if we are to fully understand the roles for different proteins in dyslipidemia and metabolic disease.

Methods

Mice

Mice with floxed alleles of the Angptl4 gene were generated by the University of Iowa genome editing facility using CRISPR/Cas9. B6SJLF1/J mice were purchased from Jackson Labs (100012; Bar Harbor, ME). Male mice older than 8 weeks were bred with 3 to 5–week–old super-ovulated females to produce zygotes for microinjection. Female ICR (Envigo; Hsc:ICR(CD-1)) mice were used as recipients for embryo transfer. Chemically modified CRISPR-Cas9 crRNAs and tracrRNAs were purchased from IDT (Alt-R CRISPR-Cas9 crRNA; Alt-R CRISPR-Cas9 tracrRNA (Cat# 1072532)). crRNA sequences were CCCTTTCACAGTCTGCTCTG and TGTGTCTAGTCTAGGAGCCG. The crRNAs and tracrRNA were suspended in T10E0.1 buffer (10 mM Tris pH 8, 0.1 mM EDTA) and combined to 1 μg/μl (~ 29.5 μM) final concentration in a 1:2 (μg:μg) ratio. The RNAs were heated at 98 °C for 2 min and allowed to cool slowly to 20 °C in a thermal cycler. The annealed cr:tracrRNAs were aliquoted to single-use tubes and stored at − 80 °C. Cas9 nuclease was also purchased from IDT (Alt-R S.p. HiFi Cas9 Nuclease). Individual cr:tracr:Cas9 ribonucleoprotein complexes were made by combining Cas9 protein and cr:tracrRNA in T10E0.1 (final concentrations: 100 ng/ul (~ 0.6 μM) Cas9 protein and 100 ng/μl (~ 2.9 μM) cr:tracrRNA). The Cas9 protein and annealed RNAs were incubated at 37 °C for 10 min. The two RNP complexes were mixed resulting in a final concentration of 100 ng/μl (~ 0.6 μM) Cas9 protein and 50 ng/μl (~ 1.5 μM) each cr:tracrRNA. Long single stranded DNA was prepared by digesting the Angptl4 target vector (524 bp 5′ arm of homology; 911 bp floxed region; 636 bp 3′ arm of homology) with the nicking enzyme Nb.Bsm1 (New England Biolabs) and purification from an alkaline-agarose gel. The final concentrations in the micro-injection mix were 20 ng/μl each cr:tracr RNA (~ 0.6 μM), 40 ng/μl Cas9 protein (~ 0.3 μM), and 10 ng/μl long ssDNA. Pronuclear-stage embryos were collected using methods described in²⁹. Embryos were collected in KSOM media (Millipore; MR101D) and washed 3 times to remove cumulous cells. Microinjection into the male pronucleus was performed and embryos incubated overnight. Two cell zygotes were implanted into pseudo-pregnant ICR females.

All pups were tested for the appropriate insertion of 5′ and 3′ LoxP sites by PCR amplification of the genomic region and subsequent sequencing. The above procedures resulted in the successful generation of a single male mouse with both 5′ and 3′ LoxP sites. This mouse was bred to a C57Bl/6 female mouse and the heterozygous progeny were interbred to generate homozygous floxed mice. During breeding, the presence of the LoxP Sites was confirmed by genotyping PCR using oligonucleotides TAGGCGCATCTACTAGGACTC (forward) and AGATATGCAAGGCTAGTGAAGAC (reverse) to detect the 5′ LoxP site and oligonucleotides CCTCCAACATCTCTTGATGTAAC (forward) and ATATGTGTATGTGACTGGATGG (reverse) to detect the 3′ LoxP site. Adipocyte-specific knockout mice (Angptl4^AdipoKO) were generated by breeding Angptl4^fl/fl mice with C57/BL6 transgenic mice containing the adiponectin promoter–driven Cre recombinase (kindly provided by Dr. Matthew Potthoff, Jackson stock 010803³⁰). The presence of adiponectin-Cre was verified by genotyping PCR using GGATGTGCCATGTGAGTCTG (forward) and ACGGACAGAAGCATTTTCCA (reverse) as primers. In all studies Cre-negative Angptl4^fl/fl littermates were used as controls.

All animal procedures were approved by the Institutional Animal Care and Use Committee at the University of Iowa and were carried out in accordance with the National Institute of Health Guide for Care and Use of Laboratory Animals. The experiments complied with the ARRIVE guidelines³¹. All animals were maintained in a climate-controlled environment at 25 °C with a 12:12 h light–dark cycle. Water was provided ad libitum. During non-fasting conditions mice were given standard mouse chow (NIH 7951) until 8 weeks of age when high-fat diet studies began. At 8 weeks of age mice were randomly assigned to either remain on standard mouse chow (NIH 7951) or given high-fat diet (60% by kCal; Research Diets, 12592). Mice were fed their respective diets for either 12 weeks or 6 months. Experiments were unblinded.

Production of Angptl4 and LPL conditioned media

A construct expressing full-length mouse ANGPTL4 (pXC4) was generated from full-length mouse ANGPTL4 cDNA (MMM1013-202763591). A V5 tag was appended to the C terminus of the open reading frame using Phusion site-directed mutagenesis (New England Biolabs) to generate a V5 tagged version of mouse ANGPTL4 (pHS5). To generate a mouse ANGPTL4 construct mimicking the predicted protein product of our Angptl4 flox allele after Cre-mediated recombination (pKMS22) we deleted residues 111–187 (Exons 2 and 3) from full-length mouse ANGPTL4 by site-directed mutagenesis. A V5 tag was appended to the new C terminus of the altered open reading frame using site directed mutagenesis (pKMS25). We also generated a mouse ANGPTL4 construct to mimic the predicted protein product of a flox allele generated by the EUCOMM/KOMP consortium and used by several previous studies^13,16,17. This flox Angptl4 allele uses a knock-out first strategy and has LoxP sites inserted into the Angptl4 gene flanking Exons 4,5, and 6. To generate a construct mimicking the predicted protein after Cre-mediated recombination (pXC32) we deleted the residues coded by exons 4 through 6 from full-length mouse ANGPTL4 by site-directed mutagenesis. A V5 tag was appended to the C terminus also using site directed mutagenesis (pXC34). To produce conditioned media containing either V5-tagged mANGPTL4, V5-tagged Flox mANGPTL4 or V5-tagged KOMP allele mANGPTL4, 293 T cells were transiently transfected with the respective constructs using the transfection agent PEI. 24 h post-transfection the media was switched to serum-free DMEM containing 1 × protease inhibitors and grown for 48 h. Mock transfected 293 T cells were used as a control. The media was then collected for use in Western blot analysis and LPL activity assays. FLAG-tagged human LPL was concentrated from the medium of a Chinese hamster ovary cell line (CHO-K1) stably expressing FLAG-tagged human LPL as previously described^32,33. The presence of LPL in the conditioned media was confirmed through Western blotting using a mouse antibody against the FLAG tag (1:5000; Sigma). LPL activity was assessed through an LPL activity assay (see below).

Western blot

Lysate and media samples collected from 293 T cells transfected with V5-tagged mANGPTL4, V5-tagged Flox mANGPTL4, or V5-tagged KOMP allele mANGPTL4 constructs were size fractionated on 12% SDS–polyacrylamide gels and then transferred to nitrocellulose membranes. Membranes were blocked with casein before primary antibodies were added (1:3000 dilution of mouse monoclonal antibody against the V5 tag (ThermoFisher MA5-15253)) in a casein buffer containing Tween. Membranes were rocked overnight at 4 °C. Following incubation, the primary antibody was removed and membranes washed 3 times with PBS containing 0.1% Tween. Membranes were then incubated with anti-mouse Dylight800-labeled secondary antibody (Invitrogen) diluted 1:5000 in casein buffer. After washing with PBS containing Tween, antibody binding was detected using an Odyssey Infrared Scanner (LI-COR).

Analysis of fasting plasma parameters

Fasting plasma parameters were measured in fasted (6 h) Angptl4^fl/fl and Angptl4^AdipoKO mice. Blood was collected into EDTA-coated capillary tubes following a tail-nick and centrifuged to collect plasma (1500 × g, 15 min, 4 °C). Plasma TG, NEFA, and glucose measurements were taken at 8 weeks of age before beginning diet and 12 weeks or 6 months following the start of diet studies. For plasma TG analysis, plasma (2 μl, technical duplicates using the same aliquot of plasma per individual mouse were used) was combined with Infinity Triglyceride Reagent (200 μl, Thermo Scientific TR22421) in a 96 well plate. Samples were incubated for 10 min at 37 °C, gently tapped to ensure proper mixing of reagent with sample, and absorbance was read at 500 nm and 660 nm. Triglyceride concentrations were determined using a standard curve prepared from Triolein standards (Nu-Chek Prep, Lot T-235-N13-Y). For plasma NEFA analysis, plasma (2 μl, technical duplicates) was combined with Color Reagent A (112.5 μl, Wako HR Series NEFA-HR 999–34691/995–34791) and incubated for 10 min at 37 °C. Following incubation, Color Reagent B was added to samples (37.5 μl, Wako HR Series NEFA-HR 991–34891/993–35191) and incubated for 5 min at 37 °C. Absorbance was read at 560 nm and 670 nm. Non-esterified fatty acid concentrations were determined using a standard curve prepared from Oleic Acid standard (TCI, O0180, Lot Z8RVM). Fasting plasma glucose concentration was measured once per mouse immediately following a tail nick using a glucometer (One Touch Ultra). Plasma amyloid A was measured using an ELISA kit (Crystal Chem #80659) following manufacturer’s protocol. Plasma activity of aspartate aminotransferase (AST, Sigma-Aldrich, MAK055) and alanine aminotransferase (ALT, Sigma-Aldrich, MAK052) were measured according to manufacturer’s protocols.

RNA extraction and qPCR analysis

Mouse tissues (heart, liver, gonadal and epididymal white adipose tissue, quadriceps muscle, subcutaneous white adipose tissue and brown adipose tissue) were harvested following a 6 h fast. Tissue was snap frozen in liquid nitrogen and stored at − 80 °C until processed. Tissues were pulverized before homogenization. Total RNA was extracted using Trizol (Invitrogen) according to manufacturer’s instructions. 2 μg of RNA was used to prepare cDNA with the High Capacity cDNA Reverse Transcription kit (Applied Biosystems, 4368813) according to manufacturer’s instructions. Prepared cDNA was used for qPCR analysis using primers across different exons of Angptl4 (Supplemental Table 1), or against Angptl4, Lpl, Ccl2, Cd68, Tnfa, Cd36, Fatp1, Fatp4, Acsl1, Acsl4, U36b4, or CycloA (Supplemental Table 2). Prepared diluted cDNA, primers, and SYBR Green ER qPCR Supermix reagent (Invitrogen, 11762100) were combined, and PCR was performed on the QuantStudio 6 Flex system (3 technical replicates per mouse, Applied Biosystems, Iowa Institute of Human Genetics). Gene expression was calculated using the ΔΔct method³⁴ using either CycloA or U36B4 as the reference gene.

DNA extraction and PCR analysis

Heart, epididymal white adipose tissue, subcutaneous white adipose tissue and brown adipose tissue were harvested from male Angptl4^fl/fl and Angptl4^AdipoKO mice and placed in ice cold PBS. DNA was extracted from approximately 25 g of tissue using a DNeasy Blood and Tissue Kit (Qiagen, 69504) according to manufacturer’s instructions. Extracted genomic DNA was amplified by PCR using primers approximately 500 basepairs upstream and downstream of the LoxP sites in the Angptl4 locus (Supplemental Table 3). Following PCR, amplified DNA was subjected to gel electrophoresis on a 2% agarose gel containing EtBr and imaged.

Preparation of ³H-labeled chylomicrons

³H-labeled chylomicrons were prepared as previously described¹⁴. Briefly, glycosylphosphatidylinositol-anchored high-density lipoprotein binding protein 1 (GPIHBP1) knock out mice were orally gavaged with 100 μCi of [9,10-3H(N)]-Triolein (Perkin Elmer, NET431001MC) suspended in olive oil. After 4 h, blood was collected via cardiac puncture and placed into a tube containing 0.5 M EDTA and placed on ice. The blood was then centrifuged at 1,500 × g for 15 min and plasma was collected. The plasma was then centrifuged at 424,000 × g twice for 2 h at 10 °C. The chylomicrons were collected from the upper layer of the resulting supernatant, resuspended in sterile saline and stored at 4 °C. Radioactivity was measured using a Beckman-Coulter Liquid Scintillation Counter.

Triglyceride uptake assay

TG clearance and uptake assays were performed in mice as previously described¹⁴. Briefly, mice were fasted for 6 h and then injected retro-orbitally with 100 μl of ³H-labeled chylomicron suspension. Blood samples were taken 1, 5, 10, and 15 min after injection. For each time point, 10 μl of blood was assayed for radioactivity in BioSafe II scintillation fluid using a Beckman-Coulter Scintillation Counter. Following the final timepoint mice were anesthetized with isoflurane and perfused with 20 mL of cold 0.5% Tyloxapol in PBS solution. Tissues (heart, liver, kidney, gonadal or epidydimal white adipose tissue, quadriceps, subcutaneous white adipose tissue, and brown adipose tissue) were harvested and weighed. 40–90 mg of each tissue was placed into a glass vial containing a 2:1 chloroform:methanol solution and stored overnight at 4 °C. 1 mL of 2 M CaCl₂ was added to each vial to separate the organic and aqueous phases. Samples were centrifuged for 10 min at 1,000 rpm and the upper aqueous layer was assayed for radioactivity in BioSafe II scintillation fluid using a Beckman-Coulter Scintillation Counter. The organic layer was allowed to evaporate overnight in an empty scintillation vial, then resuspended in scintillation fluid and counted. The counts per million (CPM) from the aqueous and organic fractions were combined to obtain the total uptake CPMs. To normalize radiolabel across mice, CPM values were normalized to the CPMs of the injected dose (measured by assaying 10% of the chylomicron suspension injected into the mouse).

Liver triglyceride measurements

Liver triglyceride measurement was performed using a modified Folch extraction method³⁵. Liver tissues (approximately 100 mg) were homogenized in 500 µl of ice-cold PBS. From this homogenate 50 µl was removed and analyzed for protein content. 1.5 ml of a 2:1 (chloroform:methanol) mixture was added to each sample. Samples were vortexed briefly and incubated for 10–15 min. Samples were then centrifuged for 10 min at 2,050 × g at 4 °C. The lower organic phase was separated with a glass Pasteur pipette and placed into a 7 mL plastic vial (RPI 125509) and allowed to dry. The dried lipid was then dissolved with 500 µl of 2% Triton X-100 in chloroform and allowed to dry. The dried lipid was resuspended in 100 µl of molecular grade water. The sample was diluted 1 to 20 for triglyceride assay analysis. Analysis was performed using 2 μl of diluted lipid (technical duplicates) which was combined with Infinity Triglyceride Reagent (200 μl, Thermo Scientific TR22421) in a 96 well plate. The plate was incubated for 10 min at 37 °C, gently tapped to ensure proper mixing of reagent with sample, and absorbance was read at 500 nm and 660 nm. Triglyceride concentrations were determined using a standard curve prepared from Triolein standard (Nu-Chek Prep, Lot T-235-N13-Y). Triglyceride levels were normalized to milligram of protein as measured in the original homogenate. Protein content was assessed by performing a DC Protein Assay (Bio-Rad) according to manufacturer’s instructions.

Lipoprotein lipase activity assays

LPL activity in tissues was measured as previously described¹⁴. Briefly, frozen tissue samples were crushed using a metal tissue pulverizer. The tissue was resuspended in LPL assay buffer (25 mM NH₄Cl, 5 mM EDTA, 0.01% SDS, 45 U/mL heparin, 0.05% 3-(N,N-Dimethylmyristylammonio) propanesulfonate zwittergent detergent (Acros Organics, 427740050)) containing protease inhibitor (Mammalian ProteaseArrest-APExBIO K1008). The tissue was then vortexed and incubated on ice for 30 min with occasional further disruption with surgical scissors. The lysate was then clarified by centrifugation at 15,000 × g for 15 min (4 °C). Protein concentrations were equalized prior to assaying activity. Supernatants were combined with a buffer comprised of 0.6 M NaCl, 80 mM Tris–HCl pH 8, 6% fatty-acid free BSA, and 1% of the EnzChek lipase fluorescent substrate (Molecular Probes, E33955). Fluorescence was measured from technical duplicates of each lysate (30 min, 37 °C) on a SpectraMax i3 plate reader (Molecular Devices). Relative lipase activity was determined following calculation of the linear slope of the curve and subtraction of background (assay buffer) slope readings. For liver lipase activity assays each lysate was treated with either vehicle (PBS) or NaCl (1 M final concentration) to differentiate the roles of hepatic lipase (NaCl insensitive) from LPL (NaCl sensitive) before the addition of the assay buffer.

The LPL activity of LPL conditioned media treated with either V5-tagged mANGPTL4, V5-tagged Flox mANGPTL4, or V5-tagged KOMP allele mANGPTL4 constructs was measured as previously described³⁶. Briefly, ANGPTL4 containing conditioned media was combined with LPL conditioned media and samples were incubated at 37 °C for 30 min. After incubation, 50 µl of each assay samples was combined with 25 µl of assay buffer (0.6 M NaCl, 80 mM Tris–HCl pH 8, 6% fatty-acid free BSA), following which 25 µl of substrate solution (1% of the EnzChek lipase fluorescent substrate (Molecular Probes, E33955) 0.05% 3-(N,N-dimethylmyristylammonio) propanesulfaonate Zwittergent detergent (Acros Organics) in 1% methanol) was then added to each sample. Fluorescence was measured from technical duplicates of each lysate (30 min, 37 °C) on a SpectraMax i3 plate reader (Molecular Devices). Lipase activity was determined as stated above.

Glucose and insulin tolerance tests

Glucose tolerance tests (GTT) were performed after fasting mice for 6 h on week 10 on diet in the 12-week diet cohort or week 24 on diet in the 6-month diet cohort. Blood samples were collected before and 30, 60, 90, and 120 min following an intraperitoneal injection with glucose (12-week HFD study: 2 g/kg for mice fed NCD, 1.3 g/kg for mice fed HFD; 6-month HFD study: 1 g/kg for all mice). For mice fed a HFD for 12 weeks, blood was collected into an EDTA-coated capillary tube and stored on ice. Plasma was collected following centrifugation of sample tubes at 1,500 × g for 20 min. Plasma glucose concentration was assessed using the Autokit Glucose kit (Wako-997–03001). 2.5 μl of plasma was combined with 200 μl of the Autokit glucose buffer solution and incubated at 37 °C for 5 min. Absorbance was read at 505 nM and 600 nM. The 600 nM reading was subtracted from the 505 nM read. Glucose concentrations were determined using a standard curve prepared from glucose standards provided by the kit. For mice fed a HFD for 6 months, blood glucose readings were taken following a tail nick, before injection and 30, 60, 90, and 120 min following glucose injection using a glucometer (OneTouch Ultra).

Insulin tolerance tests (ITT) were performed following a 4 h fast in mice following 11 weeks on diet in the 12-week diet cohort and 25 weeks on diet in the 6-month diet cohort. Glucose readings were taken following a tail-nick bleed before and 15, 30, 60, and 90 min after an intraperitoneal injection with insulin (0.75U/kg, Humalin-R 100) using a glucometer (OneTouch Ultra).

Metabolic cage studies

Mice were individually housed in Promethion cage systems from Sable Systems International at the University of Iowa Metabolic Phenotyping Core. Mice were allowed to acclimate to their housing for 48 h. Metabolic measurements were then taken for 48 h. Measurements were taken during the duration of two light cycles (6 a.m.–6 p.m.) and two dark cycles (6 p.m.–6 a.m.). Measurements were recorded as energy expenditure (kcal/hr), oxygen consumption (VO₂ (ml/min)), carbon dioxide production (VCO₂ (ml/min)) and respiratory quotient (RQ, VCO₂/VO₂).

Body composition

Body composition (fat and lean mass) was determined using nuclear magnetic resonance (NMR) in mice following 11 weeks on diet in the 12-week diet cohort and 25 weeks on diet in the 6-month diet cohort. Mice were weighed before being placed in a restraint tube without anesthesia and placed into either a Bruker LF50 (for mice under 50 g) or a Bruker LF90 (for mice over 50 g). Following NMR scanning mice were immediately returned to their cages. Body composition measurements were performed in the Fraternal Order of the Eagles Diabetes Research Center Metabolic Phenotyping Core.

Statistics and outlier identification

Results are expressed as means ± SEM. Bar graphs also show individual values. Outlier identification was performed on all mouse datasets using ROUT analysis in GraphPad Prism. An unpaired Student’s t-test with Welch’s correction was used to determine statistical significance of samples with two groups (Figs. 1 and 2). For groups of three or more statistical significance was determined by 2-way ANOVA followed by multiple comparison with Tukey correction. Repeated measured ANOVA was utilized for body weights, chylomicron clearance, GTT, and ITT assays. Statistical analysis was performed in GraphPad Prism.

Data availability

The data generated or analyzed during this study are available from the corresponding author upon reasonable request.

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Acknowledgements

This work was supported by grants from the National Institutes of Health (R01HL130146 [BSJD]). We thank the University of Iowa Genome Editing Facility for assistance in generating the ANGPTL4 floxed allele and the Fraternal Order of Eagles Diabetes Research Center Metabolic Phenotyping Core Laboratory for assistance is collecting metabolic caging data.

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Department of Biochemistry, Fraternal Order of Eagles Diabetes Research Center, and Obesity Research and Education Initiative, University of Iowa, 169 Newton Rd., PBDB 3326, Iowa City, IA, 52242, USA
Kathryn M. Spitler, Shwetha K. Shetty, Emily M. Cushing, Kelli L. Sylvers-Davie & Brandon S. J. Davies

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Kathryn M. Spitler
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Shwetha K. Shetty
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Emily M. Cushing
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Kelli L. Sylvers-Davie
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Contributions

B.S.J.D. and K.M.S. conceived the study and designed the experiments. K.M.S. conducted most of the experiments. S.K.S., E.M.C. and K.L.D.S. conducted some experiments, acquired data and gave helpful suggestions. K.M.S. and B.S.J.D. performed data analysis. K.M.S. and B.S.J.D. wrote and edited the manuscript. All authors interpreted data, participated in manuscript review, and approved the final manuscript.

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Correspondence to Brandon S. J. Davies.

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Spitler, K.M., Shetty, S.K., Cushing, E.M. et al. Regulation of plasma triglyceride partitioning by adipose-derived ANGPTL4 in mice. Sci Rep 11, 7873 (2021). https://doi.org/10.1038/s41598-021-87020-5

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Received: 17 December 2020
Accepted: 22 March 2021
Published: 12 April 2021
DOI: https://doi.org/10.1038/s41598-021-87020-5

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Subjects

Abstract

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Adipocyte Gq signaling is a regulator of glucose and lipid homeostasis in mice

Role of RAGE in obesity-induced adipose tissue inflammation and insulin resistance

Introduction

Results

Effects of adipocyte-specific ANGPTL4 deficiency on plasma TG levels and TG uptake into tissues

Effects of high-fat feeding on body phenotypes and plasma parameters in adipocyte-specific ANGPTL4–deficient mice

Effects of high-fat feeding on TG uptake and LPL activity in adipocyte-specific ANGPTL4 deficient mice

Effects of high-fat feeding on glucose tolerance and insulin sensitivity in adipocyte-specific ANGPTL4–deficient mice

Effects of adipocyte-specific ANGPTL4 deficiency in mice after a chronic high-fat diet

Discussion

Methods

Mice

Production of Angptl4 and LPL conditioned media

Western blot

Analysis of fasting plasma parameters

RNA extraction and qPCR analysis

DNA extraction and PCR analysis

Preparation of 3H-labeled chylomicrons

Triglyceride uptake assay

Liver triglyceride measurements

Lipoprotein lipase activity assays

Glucose and insulin tolerance tests

Metabolic cage studies

Body composition

Statistics and outlier identification

Data availability

References

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This article is cited by

Knockdown of ANGPTL4 inhibits adipogenesis of preadipocyte via autophagy

Suppression of angiopoietin-like 4 reprograms endothelial cell metabolism and inhibits angiogenesis

Extracellular vesicle release and uptake by the liver under normo- and hyperlipidemia

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Preparation of ³H-labeled chylomicrons