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ArticleCardiology Free access | 10.1172/JCI16751

Lipoprotein lipase (LpL) on the surface of cardiomyocytes increases lipid uptake and produces a cardiomyopathy

Hiroaki Yagyu,1 Guangping Chen,1 Masayoshi Yokoyama,1 Kumiko Hirata,1 Ayanna Augustus,1 Yuko Kako,1 Toru Seo,2 Yunying Hu,1 E. Peer Lutz,3 Martin Merkel,3 André Bensadoun,4 Shunichi Homma,1 and Ira J. Goldberg1

1Department of Medicine, Columbia University, New York, New York, USA2 Department of Pediatrics and Institute of Human Nutrition, Columbia University, New York, New York, USA3 Department of Medicine, University of Hamburg, Hamburg, Germany4 Division of Nutritional Sciences, Cornell University, Ithaca, New York, USA

Address correspondence to: Ira J. Goldberg, Department of Medicine, Columbia University, 630 West 168th Street, New York, New York 10032, USA. Phone: (212) 305-5961; Fax: (212) 305-5384; E-mail: IJG3@columbia.edu.

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1Department of Medicine, Columbia University, New York, New York, USA2 Department of Pediatrics and Institute of Human Nutrition, Columbia University, New York, New York, USA3 Department of Medicine, University of Hamburg, Hamburg, Germany4 Division of Nutritional Sciences, Cornell University, Ithaca, New York, USA

Address correspondence to: Ira J. Goldberg, Department of Medicine, Columbia University, 630 West 168th Street, New York, New York 10032, USA. Phone: (212) 305-5961; Fax: (212) 305-5384; E-mail: IJG3@columbia.edu.

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1Department of Medicine, Columbia University, New York, New York, USA2 Department of Pediatrics and Institute of Human Nutrition, Columbia University, New York, New York, USA3 Department of Medicine, University of Hamburg, Hamburg, Germany4 Division of Nutritional Sciences, Cornell University, Ithaca, New York, USA

Address correspondence to: Ira J. Goldberg, Department of Medicine, Columbia University, 630 West 168th Street, New York, New York 10032, USA. Phone: (212) 305-5961; Fax: (212) 305-5384; E-mail: IJG3@columbia.edu.

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1Department of Medicine, Columbia University, New York, New York, USA2 Department of Pediatrics and Institute of Human Nutrition, Columbia University, New York, New York, USA3 Department of Medicine, University of Hamburg, Hamburg, Germany4 Division of Nutritional Sciences, Cornell University, Ithaca, New York, USA

Address correspondence to: Ira J. Goldberg, Department of Medicine, Columbia University, 630 West 168th Street, New York, New York 10032, USA. Phone: (212) 305-5961; Fax: (212) 305-5384; E-mail: IJG3@columbia.edu.

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1Department of Medicine, Columbia University, New York, New York, USA2 Department of Pediatrics and Institute of Human Nutrition, Columbia University, New York, New York, USA3 Department of Medicine, University of Hamburg, Hamburg, Germany4 Division of Nutritional Sciences, Cornell University, Ithaca, New York, USA

Address correspondence to: Ira J. Goldberg, Department of Medicine, Columbia University, 630 West 168th Street, New York, New York 10032, USA. Phone: (212) 305-5961; Fax: (212) 305-5384; E-mail: IJG3@columbia.edu.

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1Department of Medicine, Columbia University, New York, New York, USA2 Department of Pediatrics and Institute of Human Nutrition, Columbia University, New York, New York, USA3 Department of Medicine, University of Hamburg, Hamburg, Germany4 Division of Nutritional Sciences, Cornell University, Ithaca, New York, USA

Address correspondence to: Ira J. Goldberg, Department of Medicine, Columbia University, 630 West 168th Street, New York, New York 10032, USA. Phone: (212) 305-5961; Fax: (212) 305-5384; E-mail: IJG3@columbia.edu.

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1Department of Medicine, Columbia University, New York, New York, USA2 Department of Pediatrics and Institute of Human Nutrition, Columbia University, New York, New York, USA3 Department of Medicine, University of Hamburg, Hamburg, Germany4 Division of Nutritional Sciences, Cornell University, Ithaca, New York, USA

Address correspondence to: Ira J. Goldberg, Department of Medicine, Columbia University, 630 West 168th Street, New York, New York 10032, USA. Phone: (212) 305-5961; Fax: (212) 305-5384; E-mail: IJG3@columbia.edu.

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1Department of Medicine, Columbia University, New York, New York, USA2 Department of Pediatrics and Institute of Human Nutrition, Columbia University, New York, New York, USA3 Department of Medicine, University of Hamburg, Hamburg, Germany4 Division of Nutritional Sciences, Cornell University, Ithaca, New York, USA

Address correspondence to: Ira J. Goldberg, Department of Medicine, Columbia University, 630 West 168th Street, New York, New York 10032, USA. Phone: (212) 305-5961; Fax: (212) 305-5384; E-mail: IJG3@columbia.edu.

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1Department of Medicine, Columbia University, New York, New York, USA2 Department of Pediatrics and Institute of Human Nutrition, Columbia University, New York, New York, USA3 Department of Medicine, University of Hamburg, Hamburg, Germany4 Division of Nutritional Sciences, Cornell University, Ithaca, New York, USA

Address correspondence to: Ira J. Goldberg, Department of Medicine, Columbia University, 630 West 168th Street, New York, New York 10032, USA. Phone: (212) 305-5961; Fax: (212) 305-5384; E-mail: IJG3@columbia.edu.

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1Department of Medicine, Columbia University, New York, New York, USA2 Department of Pediatrics and Institute of Human Nutrition, Columbia University, New York, New York, USA3 Department of Medicine, University of Hamburg, Hamburg, Germany4 Division of Nutritional Sciences, Cornell University, Ithaca, New York, USA

Address correspondence to: Ira J. Goldberg, Department of Medicine, Columbia University, 630 West 168th Street, New York, New York 10032, USA. Phone: (212) 305-5961; Fax: (212) 305-5384; E-mail: IJG3@columbia.edu.

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1Department of Medicine, Columbia University, New York, New York, USA2 Department of Pediatrics and Institute of Human Nutrition, Columbia University, New York, New York, USA3 Department of Medicine, University of Hamburg, Hamburg, Germany4 Division of Nutritional Sciences, Cornell University, Ithaca, New York, USA

Address correspondence to: Ira J. Goldberg, Department of Medicine, Columbia University, 630 West 168th Street, New York, New York 10032, USA. Phone: (212) 305-5961; Fax: (212) 305-5384; E-mail: IJG3@columbia.edu.

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1Department of Medicine, Columbia University, New York, New York, USA2 Department of Pediatrics and Institute of Human Nutrition, Columbia University, New York, New York, USA3 Department of Medicine, University of Hamburg, Hamburg, Germany4 Division of Nutritional Sciences, Cornell University, Ithaca, New York, USA

Address correspondence to: Ira J. Goldberg, Department of Medicine, Columbia University, 630 West 168th Street, New York, New York 10032, USA. Phone: (212) 305-5961; Fax: (212) 305-5384; E-mail: IJG3@columbia.edu.

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1Department of Medicine, Columbia University, New York, New York, USA2 Department of Pediatrics and Institute of Human Nutrition, Columbia University, New York, New York, USA3 Department of Medicine, University of Hamburg, Hamburg, Germany4 Division of Nutritional Sciences, Cornell University, Ithaca, New York, USA

Address correspondence to: Ira J. Goldberg, Department of Medicine, Columbia University, 630 West 168th Street, New York, New York 10032, USA. Phone: (212) 305-5961; Fax: (212) 305-5384; E-mail: IJG3@columbia.edu.

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Published February 1, 2003 - More info

Published in Volume 111, Issue 3 on February 1, 2003
J Clin Invest. 2003;111(3):419–426. https://doi.org/10.1172/JCI16751.
© 2003 The American Society for Clinical Investigation
Published February 1, 2003 - Version history
Received: August 26, 2002; Accepted: December 9, 2002
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Abstract

Lipoprotein lipase is the principal enzyme that hydrolyzes circulating triglycerides and liberates free fatty acids that can be used as energy by cardiac muscle. Although lipoprotein lipase is expressed by and is found on the surface of cardiomyocytes, its transfer to the luminal surface of endothelial cells is thought to be required for lipoprotein lipase actions. To study whether nontransferable lipoprotein lipase has physiological actions, we placed an α-myosin heavy-chain promoter upstream of a human lipoprotein lipase minigene construct with a glycosylphosphatidylinositol anchoring sequence on the carboxyl terminal region. Hearts of transgenic mice expressed the altered lipoprotein lipase, and the protein localized to the surface of cardiomyocytes. Hearts, but not postheparin plasma, of these mice contained human lipoprotein lipase activity. More lipid accumulated in hearts expressing the transgene; the myocytes were enlarged and exhibited abnormal architecture. Hearts of transgenic mice were dilated, and left ventricular systolic function was impaired. Thus, lipoprotein lipase expressed on the surface of cardiomyocytes can increase lipid uptake and produce cardiomyopathy.

Introduction

Lipoprotein lipase (LpL), the primary enzyme that converts lipoprotein triglyceride (TG) to FFAs, has an unusual intercellular itinerary. It is synthesized by parenchymal cells in muscle and adipose tissue, but is thought to be physiologically active only after it transfers to the endothelial cell and then undergoes transcytosis to the luminal surface. This pilgrimage is unusual in that most proteins are transferred from the circulation to the interstitial space. Both LpL and another heparin-binding protein, IL-8 (1), appear to require both proteoglycans and receptors for this process (2).

The dogma that LpL-mediated lipolysis occurs solely within the vascular lumen suggests that the pool of LpL that is found on the surface of myocytes (3) and adipocytes (4) is nonfunctional. In part, this hypothesis assumes that TG-rich lipoproteins do not leave the vascular compartment and directly interact with adipocytes and myocytes. Several recent lines of experimental evidence, however, suggest that this may be incorrect. Remnant lipoproteins have been found within the artery wall (5), and core lipids, cholesteryl ester, and retinyl esters found in lipoproteins are deposited in hearts, muscle, and adipose tissue (6). A more permeable endothelial barrier will allow this to occur, and several factors including cytokines (7) and fatty acids that result from lipolysis itself (8) enhance permeability.

To test whether LpL on the surface of cardiomyocytes can affect lipid delivery, we created a mutated LpL molecule with a cell-attachment glycosylphosphatidylinositol (GPI) anchor (Figure 1). Transfected cells produced active cell surface LpL that was released when the GPI anchor was cleaved. By creating transgenic mice expressing this protein in cardiomyocytes, we show that LpL does not have to be located on endothelial cells to function in vivo. Furthermore, GPI-anchored human LpL (hLpLGPI) transgenic mice developed a dilated cardiomyopathy with lipid accumulation within myocytes.

The hLpLGPI DNA construction. (a) The human LpL minigene with a muscle creaFigure 1

The hLpLGPI DNA construction. (a) The human LpL minigene with a muscle creatine kinase promoter was used as a template DNA for generating the hLpLGPI DNA construction. The translational start codon (ATG), stop codon (TGA), and the polyadenylation signal (PolyA) are indicated. MCK, muscle creatine kinase. (b) The hLpLGPI DNA was inserted into the plasmid containing the CMV promoter for expression in transfected cells. (c) The hLpLGPI DNA was subcloned into the plasmid containing the α-MHC promoter. The probe used for Northern blot analysis is indicated. kbps, kilobasepairs.

Methods

GPI-LpL construct. A PCR-based strategy was used to ligate the DNA sequence encoding the last 37 amino acids of membrane decay accelerating factor (DAF) (9, 10) containing the GPI-anchoring sequence to a human LpL (hLpL) minigene (11) (see Figure 1a). This strategy required the elimination of the LpL termination codon and the 3′ untranslated region. First, we performed PCR using VENT polymerase (New England Biolabs Inc., Beverly, Massachusetts, USA) with the following primers: sense primer A (5′-AGCGCTCCATTCATCTCTTCA-3′), containing a unique Eco47III restriction site in the downstream region of the hLpL minigene, and antisense primer B (5′-TTCCACTTCCTTTATTTGGGCCTGACTTCTTATTCAGAG-3′). This latter primer contains the first 19 nucleotides in the last 37 amino acids of DAF and the last 20 nucleotides, except the stop codon in the coding region of the hLpL minigene. A 639-bp fragment was produced by primers A and B with hLpL minigene as a template DNA. Second, a complementary primer to B, denoted sense primer C (5′-CTCTGAATAAGAAGTCAGGCCCAAATAAAGGAAGTGGAA-3′) and antisense primer D (5′-GATATCCTAAGTCAGCAAGCCCATGGT-3′), containing an additional EcoRV restriction site and the last 21 nucleotides in the last 37 amino acids of DAF, was used to generate a 140-bp fragment containing the entire coding sequence for the DAF GPI anchoring site by using a plasmid containing DAF cDNA as a template DNA (9). Third, the two PCR products were mixed and amplified using primers A and D to produce a 740-bp fragment containing the LpL Eco47III site, some downstream LpL sequence, and the GPI-anchoring sequence. Fourth, both this fragment and the hLpL minigene were cut with Eco47III and EcoRV, and the fragment was inserted into the minigene.

The modified LpL minigene was subcloned into the plasmid pCMV-Tag2 (Invitrogen Corp., Carlsbad, California, USA) for expression in transfected cells (Figure 1b) and was driven by the cardiac muscle–specific α-myosin heavy chain (MHC) promoter (12) for creation of transgenic mice (Figure 1c).

Cell transfection. Chinese hamster lung (CHL) cells were maintained in DMEM supplemented with 10% (vol/vol) FBS and antibiotics. CHL cells were transfected with hLpLGPI DNA by calcium phosphate, selected using G418, and identified by measuring the LpL activity in cell homogenates. LpL activity released with heparin (10 U/ml) and/or phosphatidylinositol-specific phospholipase C (PIPLC; 2 U/ml) for 30 min at 37°C was also measured.

Transgenic mice. Transgenic mice were produced that expressed hLpLGPI driven by the α-MHC promoter, and these mice were crossed with heterozygous LpL knockout (LpL1) mice (13). A second cross with LpL1 was used to produce hLpLGPI transgenics on the LpL homozygous knockout mice; this produced LpL1 littermates with or without the hLpLGPI transgene.

Lipids, FFA, and glucose. Blood from fasted (6 h) 2-month-old mice was collected from the retro-orbital plexus. VLDL, IDL/LDL, and HDL were isolated by sequential ultracentrifugation, and fast performance liquid chromatography (FPLC) analyses of plasma lipoproteins were performed as described (14). Two hundred microliters of pooled plasma from 9–11 fasted male mice was subjected to FPLC lipoprotein analyses, and cholesterol content in effluents were measured enzymatically. Cholesterol, TG, FFA, and glucose were measured as described (14). To measure tissue lipids, hearts were rapidly removed and homogenized in ice-cold 1 M NaCl buffer containing protease inhibitors to prevent TG hydrolysis. Lipids were extracted by the Bligh-Dyer method (15) using [3H]cholesterol and 10 μg β-sitosterol as internal standards. Isolated lipids were separated by thin-layer chromatography using the hexanes/diethyl ether/acetic acid (70:30:1) solvent system. Free cholesterol and cholesterol ester masses were determined by gas liquid chromatography as described (16) and were normalized for recovery of [3H]cholesterol and β-sitosterol internal standards. TG and FFA mass were determined by an enzymatic kit as described (17) and were normalized for the recovery of [3H]cholesterol. Experiments were repeated twice using four mice per group in each experiment and showed very similar results.

LpL activity. Postheparin plasma was analyzed for LpL activity as described (18). LpL activity in homogenized hearts was measured as described by Hocquette et al. (19). Fasting male mice were injected with heparin (300 U/kg, intravenously). Plasmas were obtained 10 min later and assayed in triplicate for LpL activity. The contribution of hepatic lipase was determined by assay under high-salt conditions (1 M NaCl final concentration). Human LpL was inhibited using mouse mAb 5D2, which interacts with human, but not mouse, LpL (20).

Cardiac muscle gene expression. Tissue RNA (10 μg), isolated using TRIzol reagent (Invitrogen Corp.), was subjected to electrophoresis in 1% agarose gels containing formamide and transferred to nylon filter (Hybond-N; Amersham Pharmacia Biotech Inc., Piscataway, New Jersey, USA). A 448-bp DNA fragment encoding a part of hLpL and GPI anchor (see Figure 1c) radiolabeled with [α-32P] deoxy-CTP was used for Northern analysis as reported (21). Heart RNA was also analyzed by Northern blotting using PPARα, carnitine palmitoyltransferase 1 (CPT-1), acyl-CoA oxidase (ACO), atrial natriuretic factor (ANF), GLUT4, and GAPDH probes.

Lipoprotein uptake. [3H]VLDL was produced in LpL1 mice by injection of [3H]palmitate as described (22). Fasted LpL1 and hLpLGPI/LpL1 mice were injected intravenously via jugular veins with 5.5 × 105dpm of [3H]VLDL. Eighty microliters of blood was obtained 0.5, 2, 5, and 15 min after injection. Fifteen minutes after [3H]VLDL injection, mice were perfused with 10 ml of PBS by cardiac puncture. For heparinized animals, heparin (300 U/kg) was injected intraperitoneally 10 min before [3H]VLDL injection. VLDL fraction catabolic rate (FCR) and heart uptake was determined (20).

Histology. For immunohistochemistry, hearts of 4-month-old mice were frozen in methylbutane, and LpL was detected as reported (23). Neutral lipids were assessed in hearts from mice fasted for 24 h that were perfused with PBS and embedded in Tissue-Tek OCT compound (Sakura Finetek, Torrance, California, USA). The midventricular slices of myocardium (6-μm thick) were stained with oil red O and counterstained with hematoxylin. Electron microscopy used the left ventricle fixed with 4% glutaraldehyde, postfixed in osmium tetroxide, and embedded in Epon 812. Ultrathin sections were stained with uranyl acetate and lead citrate and examined under JEM-1200ExII electron microscope (JEOL Ltd., Tokyo, Japan).

Frozen heart sections from a 3-month-old LpL1 and hLpLGPI/LpL1 mouse were used for apoptosis assays. Apoptotic cells were determined by counting TUNEL-positive nuclei (dead-end colorimetric apoptosis detection system; Promega Corp., Madison, Wisconsin, USA).

Echocardiography. Two-dimensional echocardiography was performed in conscious 6-month-old female mice using techniques described previously (Sonos 5500 system; Philips Medical Systems, Andover, Massachusetts, USA) (24). Two-dimensional echocardiographic images were obtained and recorded in a digital format. Images were then analyzed off-line by a single observer blinded to the murine genotype (25, 26).

Statistics. Data are presented as means ± SD. Student t test and ANOVA were used to compare the mean values between two and four groups, respectively. Cumulative survival rates were calculated using Kaplan-Meier survival analysis.

Results

GPI-LpL expression in CHL cells. We assessed LpL activity in wild-type Chinese hamster lung (W-CHL) and hLpLGPI-CHL cells. Both cell lines released little activity spontaneously into the medium (Figure 2). Heparin alone led to no significant increase in activity in the medium; however, PIPLC treatment released LpL activity from hLpLGPI-CHL cells (W-CHL versus hLpLGPI-CHL, 37 ± 24 versus 172 ± 25 nmol FFA/ml medium/h; P < 0.01). The combination of heparin and PIPLC led to the release of even more activity (W-CHL versus hLpLGPI-CHL, 61 ± 19 versus 494 ± 4 nmol FFA/ml medium/h; P < 0.01).

LpL activity in the medium. CHL cells were transfected with hLpLGPI DNA. LpFigure 2

LpL activity in the medium. CHL cells were transfected with hLpLGPI DNA. LpL activity in the medium released with heparin (10 U/ml) and/or PIPLC (2 U/ml) for 30 min at 37°C was measured. LpL activity was increased 4.6-fold with PIPLC and 8.1-fold with both PIPLC and heparin in the hLpLGPI-CHL cells (black bars), compared with that in W-CHL cells (white bars). Values are expressed as means ± SD. *P < 0.01.

Characterization of transgenic mice. Postheparin plasma was obtained from wild-type and transgenic mice and assayed for LpL activity. Because the effects of additional LpL in previous studies were primarily observed on the LpL-deficient background (20, 27), we crossed these mice onto the LpL1 background. No increase in postheparin plasma LpL activity was noted (Figure 3a). Moreover, plasmas were incubated with a mAb to human LpL, and no inhibition was noted (data not shown). We then assessed LpL activity in hearts of control (LpL1) and transgenic mice. One line of transgenic mice (line 357) showed a marked increase in LpL activity in the heart (Figure 3b), and we studied this line in detail. To assess whether the LpL activity in the heart was from the transgene, i.e., human and not mouse LpL, we used a mAb that does not inhibit mouse LpL (27). As shown in Figure 3c, this Ab inhibited the additional heart LpL; no LpL activity was inhibited in heart muscle homogenates from nontransgenic mice. Northern blot analysis demonstrated high expression of the hLpLGPI transgene only in the heart (Figure 3d).

LpL expression in plasma and hearts. (a) Postheparin plasma LpL activity. TFigure 3

LpL expression in plasma and hearts. (a) Postheparin plasma LpL activity. There was no difference in postheparin LpL activity between LpL1 and three lines of hLpLGPI/LpL1 mice. LpL1, n = 6; line 346, n = 3; line 357, n = 6; line 358, n = 2. (b) Heart LpL activity. Hearts from control and three lines of male transgenic animals were homogenized and assayed for LpL activity in triplicate. Homogenates of hearts of hLpLGPI/LpL1 mice (line 357, n = 3) had 3.8-fold more LpL activity than control LpL1 mice (n = 4). *P < 0.01. (c) Myocardial human LpL. Human LpL was differentiated from mouse LpL using an mAb against human LpL activity. All the additional LpL activity in hearts from hLpLGPI/LpL1 mice (line 357, n = 3) was inhibited by the Ab, and no inhibition was found when the Ab was added to homogenates from control LpL1 hearts (n = 4). The graph shows the amount of activity inhibited by the Ab. Values are expressed as means ± SD. *P < 0.01. (d) Northern blot analysis of hLpLGPI mouse tissue RNA. Ten micrograms of total heart RNA from male mice was subjected to Northern blot analysis. Probe is shown in Figure 1c. The hLpLGPI mRNA was detected only in the hearts. H, heart; M, skeletal muscle; A, adipose; Lu, lung; Li, liver; K, kidney; S, spleen. (e) Lipoprotein profiles of LpL1 and hLpLGPI/LpL1 mice. Cholesterol distribution for LpL1 mice is shown with open circles and hLpLGPI/LpL1 mice with filled circles.

Plasma lipids and lipoproteins in mice. There were no differences in plasma lipids between wild-type and hLpLGPI mice. After crossing the transgene onto the LpL1 background, male hLpLGPI/LpL1 mice (n = 11) had a nonsignificant, 25% lower average TG concentration than LpL1 mice (n = 9) (101 ± 34 mg/dl versus 126 ± 31 mg/dl; P = 0.10) due to less VLDL TG (65 ± 27 mg/dl versus 88 ± 26 mg/dl; P = 0.08); HDL levels were 39 ± 4 versus 43 ± 5 mg/dl. There were no differences in the elution of LDL or HDL when plasmas were analyzed by FPLC (Figure 3e). There were no lipid differences in female mice (TG; 100 ± 23 mg/dl in eight LpL1 mice and 97 ± 28 in 13 hLpLGPI/LpL1; HDL cholesterol was 31 mg/dl in both genotypes). Plasma FFA and glucose levels did not differ between LpL1 and hLpLGPI/LpL1 mice (data not shown).

When the transgene was bred onto the homozygous LpL-deficient mice, it did not prevent the neonatal demise of these animals; newborn knockout mice still died within 24 h. Thus, the transgene did not provide sufficient intravascular lipolysis to allow knockout mice to survive.

Lipoprotein kinetic studies. Plasma clearance of [3H]VLDL did not differ between LpL1 and hLpLGPI/LpL1 mice (FCR, 13.7 ± 6.6 and 12.1 ± 4.4 pools/h, respectively) (Figure 4a). In the presence of heparin, which normally releases LpL into the bloodstream, the transgene led to a more rapid lipoprotein-TG clearance (FCR, LpL1 versus hLpLGPI/LpL1 = 15.3 ± 6.0 versus 24.3 ± 7.4 pools/h; P < 0.02) (Figure 4b). Thus, the cardiomyocyte anchored LpL added to plasma lipoprotein clearance under these conditions. Hearts of both nonheparinized and heparinized hLpLGPI/LpL1 mice had more lipid uptake than LpL1 mouse hearts (Figure 4, c and d).

VLDL turnover studies in hLpLGPI/LpL1 mice. (a and b) Plasma VLDL clearanceFigure 4

VLDL turnover studies in hLpLGPI/LpL1 mice. (a and b) Plasma VLDL clearance without (a) and after heparin injection (b) in LpL1 and hLpLGPI/LpL1 mice. [3H]palmitate-labeled VLDL produced in LpL1 mice was intravenously injected into LpL1 and hLpLGPI/LpL1 male mice, and plasma was obtained by retro-orbital bleeds. The plasma count at 0.5 min after injection was considered as the injected dose. Plasma VLDL clearance did not differ between LpL1 (open circles, n = 9) and hLpLGPI/LpL1 mice (filled circles, n = 8). For FCR, LpL1 versus hLpLGPI/LpL1 = 13.7 ± 6.6 versus 12.1 ± 4.4 pools/h. Heparinized hLpLGPI/LpL1 mice (filled circles, n = 10) had faster clearance of radiolabeled VLDL than LpL1 mice (open circles, n = 9). For FCR, LpL1 versus hLpLGPI/LpL1 15.3 ± 6.0 versus 24.3 ± 7.4 pools/h, P < 0.02. (c and d) Heart uptake of VLDL-TG (c) and after heparin (d) from LpL1 and hLpLGPI/LpL1 mice. (c) Hearts of hLpLGPI/LpL1 (black bar, n = 8) mice had 54% more VLDL-TG uptake than control (LpL1) hearts (white bar, n = 9). LpL1 versus hLpLGPI/LpL1 = 0.016 ± 0.004 versus 0.025 ± 0.009 (heart dpm/injected dpm). (d) In the presence of heparin, hLpLGPI/LpL1 mice (black bar, n = 10) had 26% more VLDL-TG uptake in the hearts compared with control LpL1 mice (white bar, n = 9). LpL1 versus hLpLGPI/LpL1 = 0.015 ± 0.002 versus 0.019 ± 0.003 (heart dpm/injected dpm). Values are expressed as means ± SD. *P < 0.05; **P < 0.01.

The hLpLGPI mice have cardiomyopathy. To determine whether the increased lipid uptake altered heart function, we weighed hearts from LpL1 and hLpLGPI/LpL1 male and female mice. Hearts weighed 5.2 ± 0.3 mg/g body weight in LpL1 and 5.7 ± 0.4 mg/g in hLpLGPI/LpL1 mice (P < 0.01; Figure 5a).

Evidence for cardiomyopathy. (a) Heart size. Hearts were obtained from 4-moFigure 5

Evidence for cardiomyopathy. (a) Heart size. Hearts were obtained from 4-month-old male mice, and the heart weight was divided by total body weight. The hLpLGPI/LpL1 mice (filled circles, n = 11) had larger hearts (milligrams per gram body weight) than LpL1 mice (open circles, n = 11). *P < 0.02. (b and c) Survival. Breeding female hLpLGPI/LpL1 mice (n = 11) died more frequently than LpL1 female mice (n = 14); males also died more rapidly. The hLpLGPI/LpL1 males (n = 8) also died more rapidly than LpL1 male mice (n = 14). Differences among survival curves were compared using Kaplan-Meier survival analysis. *P < 0.01.

Male hLpLGPI/LpL1 mice had much greater mortality than LpL1 mice (Figure 5b). Female mice were primarily used for breeding. During a 32-week breeding period the hLpLGPI/LpL1 mice also had much greater mortality (Figure 5c; cumulative survival, hLpLGPI/LpL1 versus LpL1 = 0 versus 0.786, χ2 = 7.94; P < 0.01).

Hearts from mice expressing nonmutated human LpL had LpL protein on the surface of cells and in intracellular pools (Figure 6a). As expected, there was intense staining for human LpL protein on the cardiomyocyte surface of hLpLGPI mice (Figure 6b). Oil red O staining showed a marked increase in intracellular neutral lipid in hearts from 24 h–fasted hLpLGPI/LpL1 mice, but not in LpL1 mice (Figure 6, c and d). Electron microscopy provided further evidence that the hLpLGPI transgene led to a cardiomyopathy. Compared with LpL1 mice (Figure 6, e and f), the hLpLGPI transgenic hearts had disarrayed cardiomyocyte architecture with increased mitochondria.

(a and b) LpL immunofluorescence in the hearts. An mAb was used to detect hFigure 6

(a and b) LpL immunofluorescence in the hearts. An mAb was used to detect hLpL in hearts. In mice with transgenic expression of normal hLpL in the hearts on the homozygous LpL knockout background (He-LpL/LpL0) (28), hLpL was found in the cytoplasm and at the membrane. Hearts from hLpLGPI/LpL1 mice had intense staining for LpL on the surface of cardiomyocytes. In a, intensity of red staining is amplified tenfold compared with b. (c and d) Myocardial lipid accumulation in 24 h–fasted hLpLGPI/LpL1 mice. Oil red O staining shows an abundance of neutral lipid droplets within the cardiomyocytes of hLpLGPI/LpL1 (d) mice compared with LpL1 (c) mice. ×400. (e and f) Electron microscopy. Ultrastructure of LpL1 mouse myocardial tissues exhibited normal morphological features with well-organized myofilaments and mitochondria (e). T tubules are not visible. The hLpLGPI/LpL1 myocytes appeared severely distorted due to more mitochondria, irregular Z band of myofibrils, and dilated T tubules (f). (g) Northern blot analysis. Ten micrograms of total RNA were isolated from heart and subjected to Northern blot analysis using a part of cDNA encoding PPARα, CPT-1, ACO, ANF, and GLUT4 as probes. GAPDH is shown as a control for loading.

Apoptosis in control and hLpLGPI/LpL1 mice was assessed by TUNEL assay. A small number of TUNEL-positive cells were identified in both strains of mice, but there was no difference (data not shown).

To understand the etiology of the cardiac dysfunction, we assessed lipids and gene expression in these hearts. There was no change in TG content (0.67 ± 0.11 μg/mg heart weight in LpL1 versus 0.69 ± 0.23 μg/mg in hLpLGPI/LpL1; P = 0.9). We observed, however, a 58.9% increase in cholesteryl ester (0.40 ± 0.07 versus 0.63 ± 0.12; P < 0.05) and a 24.7% increase in FFA (125.3 ± 29.2 μmol/mg in LpL1 versus 156.2 ± 24.7 μmol/mg; P < 0.05 in hLpLGPI/LpL1 mice).

Several genes that relate to cardiac energetics were assessed by Northern blot analysis. PPARα, CPT-1, and ACO were increased (Figure 6g). ANF, a heart failure gene, was also stimulated. GLUT4 expression was decreased.

Echocardiography. The left ventricles of hLpLGPI/LpL1 mice were significantly dilated, compared with those from LpL1 mice (Table 1, Figure 7). The left ventricular systolic function of hLpLGPI/LpL1 mice was also significantly impaired. There was no increase in ventricular wall thickness, however.

Two-dimensional echocardiogram. Representative echocardiographic images froFigure 7

Two-dimensional echocardiogram. Representative echocardiographic images from LpL1 (a and b) and hLpLGPI/LpL1 (c and d) mice at end-diastole (left; a and c) and end-systole (right; b and d). The left ventricles of hLpLGPI/LpL1 6-month-old female mice were significantly larger than control LpL1 mice (see Table 1).

Table 1

Echocardiographic assessment of left ventricular geometry and systolic function in hLpLGPI/LpL1 357 transgenic line

Discussion

We created a transgenic mouse expressing hLpLGPI, and using this mouse we made several observations. (a) The hLpLGPI transgene led to large amounts of LpL activity in heart homogenates, but no active LpL was released into the bloodstream of heparinized mice. (b) Immunohistochemical studies showed large amounts of LpL protein on the surface of the myocytes. (c) Unlike heart expression of nonanchored LpL (28), the hLpLGPI transgene led to minor changes in plasma lipoproteins and did not prevent the neonatal demise of LpL knockout mice. (d) Nonetheless, cardiac uptake of lipid from circulating lipoproteins was increased in the hLpLGPI/LpL1 mice; heart uptake was also increased in heparinized hLpLGPI/LpL1 mice. (e) hLpLGPI-expressing mice had larger hearts and reduced survival after breeding. (f) Hearts of hLpLGPI mice had increased intracellular lipid, disordered cellular structure, and dilated cardiomyopathy.

Myocytes synthesize native LpL, which is then transferred to the luminal surface of capillary endothelial cells (Figure 8). Although some LpL is present on the surface of myocytes and adipocytes, it is generally thought that this represents a nonphysiologically active pool of enzyme. We created a construct in which LpL was anchored to the cell surface via a GPI anchor and showed in vitro that this construct produced active LpL. This mode of cell surface attachment was chosen because previous studies (29) had shown that a similar enzyme, hepatic lipase, was active while anchored to the cell surface via a GPI anchor. We are confident that the physiological effects of our transgene were due to myocyte cell surface LpL, and not LpL that dissociated from the cells, for several reasons: First, we found no active human LpL in the postheparin plasma of the transgenic mice despite a robust expression of activity within the heart. Second, unlike expression of nonanchored LpL, our transgene did not appreciably affect plasma lipoproteins and did not prevent the neonatal demise of LpL knockout mice. Thus, the hLpLGPI transgene was unable to hydrolyze large, nascent triglyceride-rich lipoproteins created during nursing. Third, even in the presence of heparin, a condition that releases endothelial cell–associated LpL, the hLpLGPI transgene increased uptake of circulating triglyceride into the heart.

Mechanisms of LpL mediated lipid uptake from TG-rich particles in the heartFigure 8

Mechanisms of LpL mediated lipid uptake from TG-rich particles in the heart. (a) Cardiomyocytes express LpL that dissociates from the cell surface and migrates to the luminal surface of capillary endothelial cells. At this location, LpL attaches to heparan sulfate proteoglycans (HSPG) and is able to interact with circulating TGRP. FFAs are released that cross the endothelial barrier and are acquired by myocytes. (b) Our studies show that LpL associated with the cardiomyocyte surface, in this case via a GPI anchor, also promotes lipid uptake. For this to occur, some TGRP, perhaps lipoproteins that are partially digested by endothelial-associated LpL, must exit the vasculature, enter the subendothelial space, and directly interact with cardiomyocytes. It should be noted that LpL is found on both endothelial and cardiomyocyte surfaces. Thus, the LpL-mediated interactions shown in both a and b are likely to occur in the hLpLGPI mice and may play a role in normal physiology.

Our data demonstrate that myocyte-associated LpL leads to increased lipid uptake. This finding indicated that either nonlipolyzed or partially lipolyzed particles crossed the endothelial lining of the cardiac vessels and interacted with myocyte-anchored LpL. Although data obtained more than three decades ago showed that peripheral tissues accumulate chylomicron retinyl ester, a core lipid (30), there was widespread belief that that TG lipolysis to fatty acids occurred only in capillaries and that nonhydrolyzable remnant core lipids were cleared by the liver (31). Hultin et al. (32), however, found significant uptake of core lipid from TG-rich particles into the heart and other tissues. Additionally, as shown microscopically in arteries (5), remnants can cross the endothelial barrier either due to their smaller size or because lipolysis products compromise the integrity of the endothelium (8). Thus, TG hydrolysis might not occur exclusively in the vasculature.

Immunohistological studies of hearts (3) and adipose tissue (4) have consistently shown LpL protein on the surface of myocytes and adipocytes. Moreover, adipocytes grown in culture have a significant amount of LpL on the cell surface (33). By creating mutant LpL that was bound to the surface of cardiomyocytes, we showed that LpL is functional at this site. We cannot, however, determine whether cardiomyocyte LpL requires initial lipolysis of nascent circulating lipoproteins. Although increased cardiac TG uptake was found in heparinized transgenic mice, circulating LpL in postheparin blood would initiate lipolysis of injected VLDL. The increased intravascular lipolysis in heparinized mice may have allowed more remnant lipoproteins to interact with the hLpLGPI. The more rapid VLDL FCR found after heparinization might have resulted if more VLDL interacted with LpLGPI within the subendothelial space and the partially lipolyzed particles reentered the circulation and were cleared more rapidly in the liver. We also cannot differentiate whether the greater lipid uptake in the hLpLGPI was due to lipolytic functions of the enzyme versus “bridging” functions that increase lipoprotein interaction with the cell surface (23, 34, 35). Nonetheless, our data suggest a novel pathway for cardiac fuel acquisition, cardiomyocyte LpL interaction with lipoproteins.

A second indication that the cardiomyocyte LpL was active was the unexpected development of cardiomyopathy in our mice. We have also observed dilated cardiomyopathy by echocardiography in another independent line of mice that had robust expression of the hLpLGPI transgene (line 345). This was surprising because two other transgenic mice overexpressing LpL in hearts did not have cardiomyopathy (11, 28). In these other situations the heart lipotoxicity may have been prevented by heart secretion of apoB-containing lipoproteins (17, 36). Alternatively, endothelial-associated LpL may primarily modulate plasma lipoprotein levels, whereas cardiomyocyte LpLGPI more effectively increases lipid uptake, as has been conclusively shown to occur in vitro (35).

Excess lipid uptake by hearts might occur in the setting of diabetes mellitus and has been inferred to play a role in development of diabetic cardiomyopathy (37). Obese Zucker rats also develop a cardiac lipotoxicity that might result from abnormalities in lipid uptake or oxidation due to defective leptin actions (38), this might be analogous to the dilated cardiomyopathy seen with obesity (39). Lipid-induced cardiotoxicity occurs in mice overexpressing fatty acyl CoA synthetase (40) and PPARα (37). The development of cardiomyopathy in the hLpLGPI transgenic mice conclusively demonstrates that excess cardiac lipid uptake, in addition to defective intracellular lipid metabolism, leads to cardiomyopathy. In contrast to these other models, however, we found an increased cardiac content of fatty acids and cholesteryl ester, but not stored TG. This observation, coupled with the induction of several fatty acid–metabolizing genes (CPT-1 and ACO), suggests that excess lipid oxidation is toxic. It is possible that induction of these genes might be a protective response; the cells may be attempting to maximally oxidize toxic lipid intermediates. We expect that future studies in this model and those produced by others will more precisely define the pathophysiology of cardiac lipotoxicity.

In summary, to test the hypothesis that LpL anchored to the surface of parenchymal cells was functional in vivo, we created transgenic mice in which the LpL was expressed and anchored to the myocyte surface. This LpL increased TG uptake by hearts and created a new model of cardiomyopathy. By so doing, we demonstrated that myocyte cell surface LpL, as well as LpL on the luminal endothelial surface, is physiologically significant and may contribute to cardiac energetics and, in some circumstances, cardiotoxicity.

Acknowledgments

This work was supported by grant HL45095 from the National Heart, Lung, and Blood Institute. H. Yagyu was supported in part by a grant from the Japan Health Science Foundation.

Footnotes

Conflict of interest: The authors have declared that no conflict of interest exists.

Nonstandard abbreviations used: lipoprotein lipase (LpL); triglyceride (TG); glycosylphosphatidylinositol (GPI); GPI-anchored human LpL (hLpLGPI); decay-accelerating factor (DAF); myosin heavy chain (MHC); Chinese hamster lung (CHL); phosphatidylinositol-specific phospholipase C (PIPLC); fast performance liquid chromatography (FPLC); carnitine palmitoyltransferase 1 (CPT-1); acyl-CoA oxidase (ACO); atrial natriuretic factor (ANF); heterozygous LpL knockout (LpL1); fraction catabolic rate (FCR); wild-type CHL (W-CHL); TGRP, triglyceride rich particles.

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