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International Journal of Vascular Medicine
Volume 2013 (2013), Article ID 516015, 17 pages
Myosin VI and Associated Proteins Are Expressed in Human Macrophages but Do Not Play a Role in Foam Cell Formation in THP-1 Cells
Department of Comparative Biomedical Sciences, Royal Veterinary College, Royal College Street, London NW1 0TU, UK
Received 14 February 2013; Revised 16 April 2013; Accepted 8 May 2013
Academic Editor: Karlheinz Peter
Copyright © 2013 Hayley J. Dawson et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.
Myosin VI (Myo6) functions in endocytosis in conjunction with binding partners including adaptor protein (AP)-2, disabled 2 (Dab2), and GAIP interacting protein C terminus 1 (GIPC1). This study aimed to investigate the expression and function of Myo6 in macrophages and its possible role in the endocytosis of lipoproteins during the induction of foam cell formation. Expression of Myo6, AP-2 (α2 subunit), and Dab2 in THP-1 macrophages and primary human monocyte-derived macrophages was demonstrated at the mRNA and protein level, but GIPC1 was only detected at the mRNA level. Immunofluorescence showed that Myo6 was distributed similarly to F-actin in both macrophage types. AP-2α2 was found to have a similar subcellular distribution to Myo6 and Dab2 in THP-1 cells. Myo6 was located within membrane ruffles and protrusions of the plasma membrane. These results suggest that in macrophages Myo6 is required for several functions including cell adhesion, cell progression, and macropinocytosis. Low-density lipoprotein (LDL) and oxidised LDL (oxLDL) decreased Myo6 and GIPC1 mRNA expression in THP-1 cells, but uptake of the fluorescence-labelled lipoproteins was unaffected by knockdown of the expression of Myo6 or associated proteins with siRNA. Our findings, therefore, do not support the idea that Myo6 plays a major role in foam cell formation.
The uptake of large amounts of lipids from plasma lipoproteins via endocytosis by macrophages in the artery wall to form lipid-engorged foam cells is an important initiating event in the development of atherosclerosis, a major cause of heart disease. The main lipoprotein implicated is low-density lipoprotein (LDL), but oxidative modification of the particles, a process which can occur within the vessel wall, is required before foam cell formation is induced .
The myosin superfamily is a group of actin-associated motor proteins that use ATP hydrolysis to generate force or directional movement along actin filaments [2, 3]. Many new classes of myosin have been identified since the discovery, over seventy years ago, of myosin II (“conventional” myosin), which produces contractile force in muscle cells; to date, 35 classes of myosin proteins have been characterised in mammalian cells . It is now known that these various classes of myosin motor are involved in a diverse range of intracellular processes, ranging from cell migration and division to cell anchorage and transport of cargo proteins along actin filaments . Myosin VI (Myo6), a member of the “unconventional” myosin classes, is an unusual member of the myosin superfamily in that its movement along actin filaments is towards the pointed (−) end of an actin filament, the opposite direction to myosins of other classes . For this reason, Myo6 is ideally suited for a role in endocytosis, which involves vesicle formation and/or transport away from the plasma membrane . Evidence suggests that it may play a part in organization and/or anchorage of endocytic machinery, in the provision of force required for invagination and/or vesicle fission, and during transport of vesicles through the cell cortex [6–8]. Attachment to vesicles is achieved through direct interaction with adaptor proteins (APs), including disabled 2 (Dab2) (which binds directly to receptors or indirectly via Adaptor Protein-2 (AP2)) and GAIP interacting protein C terminus 1 (GIPC1) [7–9].
Myo6 can be alternatively spliced in two regions of its cargo binding domain, giving rise to either a small insert (9aa) (SI) and/or a large insert (up to 32aa) (LI) . Thus, four variants are possible: Myo6(+SI, +LI), Myo6(−SI, +LI), Myo6(+SI, −LI), and Myo6 without inserts (Myo6(−I)) . These variants are differentially expressed and appear to have distinct cellular targets and functions [6, 7]. Although the inserts contain no functional motifs or binding sites, they may affect the structure and therefore the affinity of Myo6 for its binding partners [9, 11].
Endocytosis may occur by phagocytosis, the uptake of large particles, or by pinocytosis, the internalization of fluid and small particles [10, 12]. Phagocytosis is a regulated and selective process requiring receptor-mediated target recognition, but pinocytosis can be nonselective (macropinocytosis) or can be receptor-mediated. Clathrin-mediated endocytosis (CME) is the most studied form of receptor-mediated pinocytosis, but other forms include caveolin-mediated endocytosis, as well as clathrin-and-caveolin-independent endocytosis [10, 12]. Most evidence supporting a role for Myo6 in endocytosis relates to CME: it has been shown to colocalise with clathrin, Dab2, and AP-2 in polarised cells [13–15] and with uncoated vesicles and GIPC1 in unpolarised cells [13, 16]. In addition to CME, Myo6 has been found localized to sites of macropinocytosis in fibroblasts, and Holt et al.  have reported that loss of Myo6 function in bone marrow-derived murine dendritic cells causes enhancement of macropinocytotic uptake, but its exact function in this process remains unclear [7, 18].
Given the importance of endocytosis in the uptake of lipoproteins by macrophages, it is possible that Myo6 may have a role in foam cell formation and thus play a part in atherogenesis. Little is known, however, about the expression and function of Myo6 and its binding partners in macrophages.
Expression of Myo6 , Dab2 , and AP-2  has been detected in murine macrophages and expression of GIPC in human peripheral blood monocytes , but, except for one report which found Myo6 mRNA in macrophages derived from the human monocyte cell line, THP-1 , no information is available on expression of these proteins in human macrophages. Moreover, as far as we are aware, splice variant expression, subcellular localisation, and protein-protein interactions of Myo6 have not been studied previously in any macrophage type.
The aims of this study were to investigate the expression and function of Myo6 and related proteins in human macrophages and to test the hypothesis that Myo6 plays a role in the endocytosis of LDL and/or oxLDL by these cells. Expression of Myo6 (including splice variants), Dab2, AP-2α2 (one of the large subunits of the AP-2 heterotetrameric complex), and GIPC1 was demonstrated in both THP-1 macrophages and primary human monocyte-derived macrophages (HMDM), and their subcellular location and interactions within the cells were investigated. To study the possible role of these proteins in macrophage endocytosis, THP-1 macrophages were used to evaluate the effects of LDL and oxLDL on the expression of mRNA and protein for Myo6, Dab2, AP-2, and GIPC1, as well as the effects of inhibition of Myo6 and Dab2 expression by small interfering RNA (siRNA) on the uptake of the lipoproteins by the cells. The THP-1 cell line was established 30 years ago, and since then it has been used very extensively to study the role of monocyte/macrophages in cardiovascular disease. A recent comprehensive review of the value of this model  concluded that, in defined conditions, THP-1 cells resemble HMDM and mimic the changes seen in atherosclerosis and that, provided results are interpreted cautiously, they are suitable for the study of the mechanisms by which these cells affect vascular function. The present work shows that the expression and subcellular location of Myo6 and related proteins are generally similar in HMDM and THP-1 macrophages, but because of the practical difficulties in obtaining large numbers of HMDM, it was not possible to use primary cells in all of our experimental approaches.
2. Materials and Methods
Fetal bovine serum and penicillin/streptomycin were obtained from Gibco (Paisley, UK), and DMEM and L-glutamine were from PAA UK (Yeovil, UK). RPMI 1640 medium, β-mercaptoethanol, 4β-phorbol 12 myristate 13-acetate (PMA), Oil Red O, ethidium bromide, and fluorescein-isothiocyanate- (FITC-) conjugated goat anti-mouse IgG were supplied by Sigma Aldrich (Poole, UK). 4′,6-diamidino-2-phenylindole (DAPI) 1,1′-dioctadecyl-3,3,3′3′-tetramethylindo-carbocyanine perchlorate (DiI), rhodamine conjugated phalloidin, Alexa488 conjugated goat anti-rabbit-, and Alexa555 donkey anti-rabbit IgG were purchased from Invitrogen Molecular probes (Paisley, UK). Myo6 (H-215) and Dab2 (H-110) rabbit polyclonal IgG and normal donkey serum were from Santa Cruz Biotechnology Inc. (Heidelberg, Germany). Other antibodies including mouse polyclonal anti-AP-2α2 and rabbit polyclonal anti-β-microglobulin IgG (Abcam, Cambridge, UK), mouse polyclonal anti-GIPC1 IgG (Abnova, Heidelberg, Germany), rabbit polyclonal anti-β-actin (Cell Signaling Technology, Hitchin, UK), and horse radish peroxidase-conjugated goat anti-mouse and goat anti-rabbit IgG (Thermo Fisher Scientific, Cramlington, UK) were from various suppliers as indicated, and normal goat serum was from Dako UK Ltd (Ely, UK).
2.2. Culture of THP-1 Macrophages, HMDM and COS-7 Cells
THP-1 monocytes were cultured in suspension in RPMI-1640 media, supplemented with 10% heat inactivated (56°C, 30 min) fetal bovine serum (FBS), 1% penicillin/streptomycin, and 0.1% β-mercaptoethanol (culture medium). For differentiation into macrophages, monocytes were incubated with 200 ng/mL phorbol 12-myristate 13-acetate (PMA) (200 ng/mL) for 72 h. Prior to experimental treatment, the medium containing PMA and nonadherent or dead cells was removed, the cells were washed twice, and fresh culture medium was added. Cells were incubated with or without treatment for up to 5 days, with media changes every 48 h.
For HMDM preparation, primary human monocytes were isolated from the blood of healthy adult volunteers with ethical approval from the East London Research Ethics Committee. Blood was collected into tubes containing 15% EDTA (v : v) and processed immediately by the addition of PBS (1 : 1, v : v), layering over 15 mL Lymphoprep (Axis Healthcare Ltd, Borehamwood, Herts, UK) and centrifugation at 800 ×g (30 min, 20°C). The mononuclear cell layer was collected, mixed with an equal volume of ice-cold PBS containing 0.4% (v/w) trisodium citrate, and centrifuged at 800 ×g (5 min, 4°C). After removal of the supernatant, the cell pellet was re-suspended in 0.2% (w : v) NaCl for 30 sec at 4°C to lyse any remaining red blood cells and 1.6% (w : v), NaCl was added, and the tubes were centrifuged as previously mentioned. Resuspension in PBS containing 0.4% (w : v) trisodium citrate and centrifugation were then repeated ×6 to remove contaminating platelets. The final pellet was resuspended in RPMI-1640 medium containing 5% FBS and 1% penicillin/streptomycin, and the cells were incubated at 37°C in 5% CO2 for 7 days to allow differentiation into macrophages. Examination by light microscopy indicated that the cells showed a macrophage phenotype after 6 days; cells were used on the 7th day after washing with PBS (×4) to remove any remaining nonadherent cells.
COS-7 adherent cells were cultured in DMEM maintenance media supplemented with 10% FBS, 1% penicillin/streptomycin, and 1% L-glutamine.
2.3. mRNA Analysis
Total RNA was extracted from HMDM, THP-1 macrophages, and COS-7 cells using an extraction kit (Sigma-Aldrich, Poole, UK) and RNase-free DNase (Qiagen, Crawley, UK) as recommended by the manufacturers. For reverse transcription, RNA (1 μg) was used to generate cDNA using Omniscript Reverse transcriptase (Qiagen) and Oligo-(dT) primers according to the manufacturers’ instructions. For expression studies in untreated cells, PCR was used to amplify gene products for Myo6, the small and large insert regions of Myo6, Dab2, AP-2α2, GIPC1, and in GeneAmp PCR System 9700 (Applied Biosystems) using the primers shown in Table 1 and the following protocol: denaturing at 95°C (5 min), followed by 35 cycles consisting of 30 sec at 94°C, 90 sec at the appropriate specific annealing temperatures and extension at 72°C for 60 sec, with a final extension at 72°C for 10 min. Product sizes and annealing temperatures are shown in Table 2. PCR products were visualised on 1.2% or 3% agarose gels containing 0.01% ethidium bromide (v : v). Gels were viewed and photographed under UV light using the ChemiDoc XRS scanner (Bio-Rad, Hemel Hempstead, UK).
To determine the effects of LDL or oxLDL on mRNA expression, THP-1 macrophages were incubated with the lipoproteins (50 μg protein/mL) for 8 or 24 h, and total RNA was then extracted and reverse transcribed as described previously. The abundance of mRNA transcripts for Myo6, Dab2, AP-2α2, GIPC1, β-actin, β2-macroglobulin, and ribosomal protein L13a was assessed by quantitative PCR (qPCR) in an Opticon 2 LightCycler system (MJ Research, Waltham, Massachusetts, USA) using the primers shown in Table 1 employing the following protocol: denaturing at 94°C (2 min), followed by 37 cycles of amplification consisting of denaturation at 94°C (15 sec), incubation at an appropriate, specific annealing temperature (1 min), followed by extension at 72°C (1 min). Threshold cycle values were determined using Opticon Monitor 3 software and quantified using the standard curve for each gene. Normalisation factors (NF) were calculated from the geometric means of the three most stably expressed reference genes (β-actin, β2-macroglobulin, and ribosomal L13a protein) as determined using geNorm software or, for siRNA studies, to the reference gene β2-microglobulin run on the same qPCR plate with its own standard curve. In the latter case, annealing temperatures (Table 1) were adjusted to a temperature suitable for both the genes of interest and β2-microglobulin.
2.4. Western Blotting
For analysis of protein expression by Western blotting, cells were washed twice with PBS and treated with RIPA lysis buffer (150 mM NaCl, 50 mM Tris (PH 8.0), 1% Triton X-100, 0.5% deoxycholate (DOC), 0.1% SDS) containing protease inhibitor cocktail (10 μL/mL) (5 min, 4°C). Lysates were agitated for 30 min at 4°C, centrifuged at 93 ×g (10 min at 4°C) to remove cell debris, and then denatured and reduced in NuPAGE LDS Sample Buffer (2 : 1, v : v) containing 10% β-mercaptoethanol solution at 70°C for 10 min. Proteins (10–30 μg) were separated by SDS-polyacrylamide electrophoresis (8% or 10% resolving gel with 5% stacking gel or precast Mini-PROTEAN TGX BioRad graded gels (4–15%) (BioRad)) and transferred to polyvinylidene fluoride (PDVF) membranes. Blocking was carried out in 5% (w : v) nonfat milk powder at room temperature for 1 h, and membranes were then incubated with polyclonal rabbit anti-Myo6 (1 : 200), anti-Dab2 (1 : 400), anti-β-actin (1 : 1,000) or anti-β-microglobulin (1 : 700), or mouse anti-GIPC1 (1 : 500) IgG overnight at 4°C with agitation. After washing in TBST (4 × 15 min), horseradish peroxidase-conjugated goat anti-rabbit or anti-mouse secondary antibodies (β2-microglobulin, Dab2, Myo6, 1 : 8,000; β-actin, GIPC1, 1 : 10,000) were added and incubations were continued for 1 h at room temperature with agitation. Finally membranes were washed in TBST (4 × 15 min) and bands were visualized using enhanced chemiluminescence (GE healthcare, Little Chalfont, UK). Band densities were digitized from film to 12 bit images using a ChemiDoc XRS (Bio-Rad) and quantified as mean grey values measured over identical areas using Quantity One software (Bio-Rad). Results are shown relative to the control sample in each case.
2.5. Confocal Laser Scanning (CLS) Fluorescence Microscopy
CLS fluorescence microscopy was conducted using either a Leica SP5 or a Zeiss LSM510 confocal microscope. For all experiments, THP-macrophages or HMDM were incubated in 24-well plates containing coverslips, which were removed for mounting at the end of the procedure. Coverslips were washed twice in 1 × PBS, fixed with 4% formalin (v : v) for 15 min, and followed by cell permeabilisation in 0.25% Triton X-100 for 5 min prior to blocking (1 h, 3% (w : v) BSA) with normal goat (NGS) or donkey (NDS) serum (1% w : v). IgG polyclonal rabbit anti-Myo6, -GIPC1 (1 : 100, v : v), -Dab2 (1 : 200, v : v), or polyclonal mouse anti-AP-2α2 (1 : 100, v : v) (diluted in 0.1% (w : v) BSA and 1% NGS/NDS in PBS) was then added. After 1 h, cells were washed (0.5% BSA in PBS, 5 min × 4 and 15 min × 1) and incubated with IgG polyclonal secondary antibodies conjugated to a specific fluorochrome as follows: goat anti-rabbit antibody conjugated to Alexa Fluor 488 (1 : 1,000, v : v), donkey anti-rabbit antibody conjugated to Alexa Fluor 555 (1 : 1,000, v : v), or goat anti-mouse antibody conjugated to Fluorescein Isothiocyanate (FITC) (1 : 25, v : v) dilutions in 0.1% BSA and 1% NGS in PBS (w : v). Where double immunofluorescence staining was used, compatible pairs of primary or secondary antibodies were incubated with cells simultaneously. Cells were then washed in PBS (5 min × 3, then 15 min × 1).
To visualise cell nuclei, cells were incubated (3 min) with 300 nM 4′,6-diamidino-2-phenylindole (DAPI), a nucleic acid stain. The structure of F-actin was preserved prior to visualisation, with minimal loss of free myosin, by incubating cells (45 sec) with buffer containing NaCl, 137 mM; KCI, 5 mM; Na2HPO4, 1.1 mM; KH2PO4, 0.4 mM; NaHCO3, 4 mM; glucose, 5.5 mM; MgCl2, 2 mM; EGTA, 2 mM; PIPES, 5 mM; pH 6.0-6.1 [25, 26] supplemented with 0.32 M sucrose, 0.1% Triton X-100, and 1 μg/mL phalloidin . Cells were immediately incubated with 165 nM phalloidin conjugated to rhodamine, as a fluorescent marker (20 min). Phalloidin binding to actin stabilises the filament, preventing depolymerisation. To remove residual counterstain, cells were washed twice in PBS before mounting. Areas of fluorescence signal were detected by application of a threshold and the mean fluorescence intensity quantified using Volocity (5.4) 3D image analysis software (PerkinElmer, Waltham, MA, USA).
2.6. Low-Density Lipoprotein (LDL) Isolation and Modification
LDL (–1.063 g/mL) was isolated from human plasma obtained from the National Blood Service (North London, UK), using sequential density gradient ultracentrifugation. Final preparations of native LDL (nLDL) were dialysed against 0.9% NaCL (w/v) containing 10 μM EDTA (5L × 4). For LDL used in oxidation studies, EDTA was omitted. Lipoproteins were stored at 4°C, protected from light and under argon gas. Human plasma was used within 1 month of purchase and LDL within 2 weeks of isolation.
LDL was oxidised by incubation with CuSO4 (5 μM) for 6 h, oxidation was terminated by the addition of EDTA (1%, 50 μL/mL v/v), and the extent of oxidation was assessed by measuring the concentration of malondialdehyde (MDA) (nmol/mg LDL protein) using the Thiobarbituric Acid Reactive Substances (TBARS) assay . CuSO4 was removed by dialysis at 4°C against 0.9% NaCl (w/v) containing 10 μM EDTA (5L × 4). Both nLDL and oxLDL were sterilised by passage through a 0.45 μm filter.
For labelling of nLDL and oxLDL with the fluorescent probe 1,1′-dioctadecyl-3,3,3′,3′-tetramethylindo-carbocyanine perchlorate (DiI), lipoprotein deficient serum (LPDS), prepared from human plasma by sequential density gradient ultracentrifugation, was added to the LDL preparations (1 mg LDL protein/2 mL LPDS) followed by DiI (300 μg DiI/mg LDL protein). To prevent oxidation, EDTA was added to the preparations at a final concentration of 10μM, and the mixture was incubated for 8 h at 37°C with shaking. The DiI labelled lipoproteins (DiI-nLDL/oxLDL) were then isolated by ultracentrifugation at 1.063 g/mL (96,919 ×g, 15 h, 4°C) and dialysed as described previously before use.
2.7. siRNA Studies
Small interfering RNA (siRNA) sequences designed to target Myo6 (combination of two sequences), Dab2, AP-2α2 (Table 2), or GIPC1 (sequence not released by the manufacturer) were used to inhibit the expression of their cognate genes. THP-1 macrophages (6 × 105 well) were transfected with siRNA using HiPerFect transfection reagent (Qiagen, Crawley, UK). 5 nM (AP-2α2, GIPC1, Dab2) or 40 nM (Myo6) siRNA was added to 100 μL RIPA-1640 medium, then 20 μL HiPerFect was added, and the mixture was incubated for 10 min at room temperature to allow siRNA-HiPerfect complexes to form prior to their addition (100 μL) to cells. In all experiments, a nonsilencing scrambled siRNA (AllStars negative control, Qiagen), which has no known homology to any mammalian genes, was used as a control. To assess the effects of inhibition of gene expression on the uptake of nLDL and oxLDL by THP-1 macrophages, lipoproteins were labelled with the fluorescent probe DiI and uptake was assessed using fluorescence wide-field microscopy. Cells were seeded in 24-well plates (1.6 × 105 cells/well) and incubated with siRNA for 48–72 h. DiI-labelled LDL or oxLDL (50 μg protein/mL) was then added, and the incubations, continued for periods up to 24 h. Cells were fixed and imaged using a Leica inverted DMRIB wide-field microscope.
2.8. Analytical Methods
Protein concentrations of cell lysates were determined by the method of Lowry  and those of nLDL and oxLDL were obtained using Peterson’s modification of Lowry’s method . The total cholesterol content of lipoproteins was determined by enzymatic analyses using commercially available kits (Thermo Fisher Scientific, Cramlington, UK). Statistical analysis was performed using Student’s test or one- or two-way ANOVA (followed by Bonferroni’s multiple comparison test), as indicated in the text.
3.1. Expression of Myo6 and Associated Proteins AP2, Dab2, and GIPC1 in THP-1 Macrophages and HMDM
To determine whether Myo6 and its binding partners are expressed in macrophages, total RNA was isolated from untreated THP-1 macrophages and HMDM and then used to generate cDNA for amplification of gene products by conventional PCR. Bands at the expected product size (Table 1) were detected for Myo6 (Figure 1(a)) and also for Dab2 (Figure 1(b)), the large subunit of AP-2, AP-2α2, which was used to detect AP-2 expression (Figure 1(c)) and GIPC1 (Figure 1(d)). In all cases, no bands were found for any of the genes when PCR was carried out in the absence of either primers (data not shown) or cDNA. These results demonstrate that both THP-1 macrophages and HMDM express mRNA encoding Myo6, Dab2, AP-2α2, and GIPC1.
Although previous studies in mammalian cells have established that Myo6 can be expressed as four variants due to alternative splicing of the LI and SI regions of the tail domain [6, 11], it is not known which splice variants are expressed in macrophages. Dance et al.  demonstrated the presence of Myo6 both with and without the LI and SI in COS-7 cells, and we have used the same primer sequences to investigate their expression in THP-1 macrophages and HMDM. We found bands identical to those reported by Dance et al.  for Myo6 variants in COS-7 cells (Figure 2), and these were used as markers of band identity. Figure 2 shows that bands corresponding to Myo6(−LI) (Figure 2(a)) and Myo6(−SI) (Figure 2(b)) in COS-7 cells were also found in THP-1 macrophages (Figures 2(a) and 2(b), white arrows). A band of product size equivalent to Myo6(+SI) mRNA (Figure 2(b), green arrows) was also detected in THP-1 cells, although at a lower level relative to Myo6(−SI) in comparison to COS-7 cells. Expression of Myo6(+LI) was low in COS-7 cells, but a band corresponding to this variant was clearly present in THP-1 macrophages, and these cells also expressed number of other transcripts of larger size (Figure 2(a), blue arrows). HMDM showed similar patterns of expression of Myo6 splice variants to those observed in THP-1 cells, with Myo6(−LI) and multiple bands of Myo6(+LI) (Figure 2(c)) and Myo6(−SI) (Figure 2(d)) present; however, Myo6(+SI) was not detected in these cells (Figure 2(d)).
Immunoblotting indicated the presence of a protein of the molecular weight of Dab2 (96/67 kDa) in 3 lysates from THP-1 macrophages and in cells from 3 individual donors for HMDM. Images from a representative experiment are shown in Figure 3(a). In addition, a band corresponding to the molecular weight of Myo6 was clearly present in 3 lysates of THP-1 cells (one example is shown in Figure 3(b)). For HMDM, a weak band corresponding to Myo6 was visible in cells from 2 donors when 45 μg protein was loaded (one example is shown in Figure 3(b)) but not when a lower amount of protein (35 μg) was used (data not shown). The expression of Myo6 in HMDM, however, was clear in the immunofluorescence experiments described later.
We were unable to demonstrate the presence of GIPC1 protein definitively. In addition, AP-2α2 protein could not be detected by immunoblotting, although its presence in THP-1 macrophages was demonstrated by immunofluorescence (see later).
3.2. Subcellular Localisation of Myo6 and Associated Proteins in THP-1 Macrophages and HMDM
Immunofluorescence was used to explore the distribution and interactions of Myo6 and associated proteins in THP-1 macrophages and HMDM. The proteins were detected using Alexa488- (Myo6, Dab2) or FITC-(AP-2α2) conjugated secondary antibodies (green) and where appropriate, DAPI (blue) and rhodamine-conjugated phalloidin (red) were employed as counterstains for the nucleus and F-actin, respectively. No green fluorescence was observed in negative controls when cells were incubated with FITC- or Alexa488-conjugated secondary Ab in the absence of the primary antibodies.
AP-2α2 and Dab2 were located mainly around the cell periphery in a punctate staining pattern in both THP-1 macrophages (Figures 4(a) and 4(c)) and HMDM (Figures 4(b) and 4(d)). By contrast, Myo6 was found to exhibit a more diffuse staining in both cell types (Figure 5) and was found within membrane protrusions and membrane ruffles along the leading edge of the cells (THP-1 cells Figures 5(a), and 5(b), HMDM, Figures 5(c) and 5(d)).
Association between Myo6 and F-actin was studied using fluorescence labelling techniques in both THP-1 macrophages and HMDM (Figure 6). Confocal images showed that, as expected, Myo6 appeared to be associated with F-actin, with similar distributions mainly found around the cell periphery in both types of macrophages (Figures 6(a)(ii) and 6(b)), including possible podosome attachment sites in THP-1 cells (Figure 6(a)(i)). To assess the extent of interaction between Myo6 and AP-2α2, double immunofluorescence experiments were carried out in THP-1 macrophages in which Myo6 was labelled with Alexa555-linked secondary antibody to give red fluorescence (Figure 7(a)). AP-2α2 immunofluorescence was observed mainly at the cell periphery, while that for Myo6 was also found intracellularly (Figure 6(a)). Regions of overlap were rare and imperfect (Figure 7(a)(ii)), suggesting that the two proteins are not substantially associated within the cells. Experiments using an Alexa555-linked secondary antibody for Dab2, however, indicated that there was substantial colocalisation between AP-2α2 and Dab2 (Figure 7(b)).
3.3. Effects of LDL and oxLDL on the Expression of Myo6 and Related Proteins in THP-1 Macrophages
The compositions (protein, total cholesterol, and TBARS content) of the nLDL and oxLDL preparations used are shown in Table 3. No significant differences were found in the protein or total cholesterol content of nLDL as compared to oxLDL. The concentration of TBARS, however, was approximately 19-fold higher in oxLDL, indicating a significantly increased oxidative state.
THP-1 macrophages were incubated with or without nLDL or oxLDL (50 μg protein/mL) for 8 h or 24 h, and lysates were then used to determine the abundance of transcripts for Myo6, Dab2, AP-2α2, and GIPC1 by a combination of RT-qPCR and immunoblotting (the latter for Myo6 and Dab2). Incubation with nLDL caused no significant change in Myo6 or Dab2 mRNA levels at either time point (Figures 8(a) and 8(b)). mRNA abundance for AP-2α2, however, was decreased by about 35% after 24 h () and that for GIPC1 by 31% after 8 h () or 39% after 24 h () (Figures 8(c) and 8(d)). oxLDL, however, caused a marked decrease in mRNA levels for Myo6 at both time points (8 h, −47%, ; 24 h, −61%, ) and also significantly reduced mRNA levels for AP-2α2 (−39%, ) and GIPC1 (−22%, ) compared to control values.
Myo6 and Dab2 protein concentrations showed little change when macrophages were incubated with either nLDL or oxLDL, with a small decrease in Dab2 (−19%) in the presence of nLDL being the only difference from control values (Figures 8(e)–8(h)). Myo6 proteins levels, however, were significantly lower after treatment with oxLDL as compared to nLDL after 8 h (+47%, , Figure 8(f)), while Dab2 levels were significantly higher (+24%, , Figure 8(h)).
3.4. siRNA Studies
The effects of inhibition of the expression of Myo6, Dab2, AP-2α2, and GIPC1 on the uptake of nLDL and oxLDL by THP-1 macrophages were studied using siRNA sequences designed to target their cognate genes. mRNA abundance for all test proteins was maximally decreased in THP-1 macrophages 24–48 h after transfection with antisense oligonucleotides as compared to scrambled controls (reduction in abundance was −75–85%, Myo6, Dab2, and AP-2α2, ; −50% GIPC, ) (Figures 9(a)–9(d)). After 72 h (AP-2α2) or 96 h (Myo6 and Dab2), however, the inhibitory effect was reduced for all genes except GIPC1. In addition, protein concentrations of Myo6 were reduced by 75–83% between 48 and 96 h and those for Dab2 by >75% between 24 and 96 h () (Figures 9(e) and 9(f)).
Uptake of nLDL and oxLDL by THP-1 macrophages was measured using DiI-labelled lipoproteins (50 μg/mL) and fluorescence microscopy. In non-siRNA-treated cells, the area of fluorescence signal increased between 2 h and 24 h, and, as expected, the rate of increase was faster with oxLDL as compared to nLDL (Figures 10(a) and 10(b)). Comparison of the areas of fluorescence signal in macrophages transfected with scrambled siRNA, or siRNA targeting Myo6 showed no significant differences (Figures 10(c) and 10(d)); similar results were obtained when siRNA targeting Dab2, AP-2α2 or GIPC1 were used (data not shown).
Myo6 is an intracellular motor protein found to be associated with F-actin in the cytoskeleton [7, 31]; in cells where it functions in endocytosis, it is also found in association with other proteins that have assigned roles in endocytosis, namely, AP-2, Dab2, and/or GIPC1. Myo6 and the interactive adaptor proteins Dab2, AP-2, and GIPC1 are widely expressed and play diverse, often essential, roles in cellular functioning and signalling. Furthermore, these proteins have been shown to function and interact during CME, and Myo6 is thought to provide a driving force for vesicle formation and trafficking . However, although the endocytosis of lipoproteins by macrophages to form foam cells is crucial to atherosclerotic development, the potential roles for Myo6 and binding partners in this process have not been explored till now. Indeed, little information is available about the expression of these proteins or their roles in human macrophages, and nothing is known about their subcellular location or mutual interactions in these cells.
We have demonstrated the mRNA expression for Myo6, Dab2, AP-2, and GIPC1 in primary human macrophages (HMDM) as well as in macrophages derived from the human monocyte cell line, THP-1 (Figure 1). Furthermore, the presence of Myo6, Dab2, and AP-2 protein was demonstrated in these two cell types using both immunoblotting and immunofluorescence (Figures 3–5). Previous studies have detected Dab2 mRNA in mouse bone marrow macrophages and Myo6, Dab2, and AP-2 protein in various murine macrophage cell lines [19–21, 32]. In addition, Myo6 mRNA  and low levels of GIPC1 mRNA  or protein  have been found in human peripheral blood leukocytes. Nonetheless, this is the first report of the expression of these proteins in human macrophages, except for one study showing Myo6 mRNA expression in THP-1 cells .
As positive controls, we demonstrated splice variant expression of Myo6 in COS-7 cells, previously shown to express Myo6 with and without the LI and SI insert sequences . THP-1 macrophages and HMDM were found to express Myo6(−LI), but while only one weak band corresponding to Myo6(+LI) was observed in COS-7 cells, numerous bands in this region were seen within the two macrophage cell lines (Figures 2(a) and 2(c)). Dance et al.  found a similar pattern of multiple bands for Myo6(+LI) in the epithelial cell lines ARPE-19 and LLC-PK1 and determined that these resulted from alternative splicing within the LI region. Expression of Myo6(−SI) was demonstrated in THP-1 macrophages and HMDM in our experiments (Figures 2(b) and 2(d)), but although Myo6(+SI) was clearly present in THP-1 cells, its expression was not detected in HMDM. Alternative splice variants of Myo6 are differentially expressed and have distinct subcellular locations and functions in various cell types. In polarised epithelial cells, for example, Myo6(−LI) has been shown to associate with uncoated endocytotic vesicles via GIPC1, while Myo6(+LI) is recruited to clathrin coated pits/vesicles via Dab2 . Thus, the expression of various Myo6 splice forms in human macrophages further indicates that Myo6 is likely to have multiple functions, including CME, within these cells .
In the current study, Myo6 was found to be distributed throughout the cytoplasmic pool in both THP-1 macrophages and HMDM, with particular localisation to actin-generated protrusions of the plasma membrane, and possibly membrane ruffles (Figure 5), often expressing a punctuate pattern in the cell periphery indicative of association with vesicular structures, as noted previously [6, 14, 15]. As expected, Myo6 appeared to be associated with F-actin, particularly at the apical membrane and at putative podosome attachment sites (Figure 6). Similar associations of Myo6 to plasma membrane protrusions and membrane ruffles have been reported in a number of migratory cell types other than macrophages, including epithelial, fibroblast, and ovarian border cells [13, 35], suggesting that it plays an important part in the coordination of the various processes required for cell migration, including cell adhesion and directed cell progression. Chibalina and colleagues  have demonstrated that Myo6 functions in endocytosis and vesicle recycling in such cells, and in conjunction with GIPC, it has also been shown to participate in the endocytosis of activated α5β1 integrin , which links it directly to focal adhesion turnover. Buss et al.  have also suggested that the association of Myo6 with membrane ruffles in fibroblasts may be indicative of a role in macropinocytosis.
During CME, AP-2 is known to act in the formation of clathrin-coated pits/vesicles , while Dab2 can either associate with AP-2 as an accessory protein  or act as an adaptor protein in its own right . Dab2 also has numerous functions outside of CME, and so the extent of its association with clathrin-coated vesicles varies between cell types [40, 41]. In this study CLS fluorescence microscopy was used to show that AP-2α2 and Dab2 (Figure 4) are located adjacent to the periphery of both THP-1 macrophages and HMDM in a punctate staining pattern, indicative of vesicle association.
To assess the extent of interaction between Myo6, Dab2, and AP-2α2 in THP-1 macrophages, double immunofluorescence labeling experiments were used. Dab2 and AP-2α2 were shown to be partially colocalised (Figure 7(b)) in a punctate pattern, indicative that Dab2, the direct binding partner of Myo6, is associated with clathrin-coated pits/vesicles in THP-1 macrophages. This finding is consistent with previous work showing that Dab2 is associated with AP-2α2 in COS-7 cells . However, although association between Myo6 and AP-1 has been reported in other cell types , the present experiments suggest that the two proteins do not have substantially overlapping distributions in macrophages (Figure 7(a)).
Having shown that Myo6, Dab2, AP-2, and GIPC1 are expressed in human macrophages and that there are some interactions between them, we explored the possibility that they might play a part in macrophage foam cell formation. THP-1 macrophages were used for these studies since there are serious technical difficulties in obtaining sufficient HMDM for the types of experiment needed. These cells have some advantages over HMDM in that, because they are genetically homogeneous, there is less variability in their phenotype, and they can be stored indefinitely at −80°C. Another factor which was important for our experiments is that transfection efficiency of THP-1 macrophages with siRNA is much greater than that with HMDM.
The uptake of nLDL and oxLDL by macrophages is known to be mediated by different receptors: nLDL undergoes endocytosis via the LDL receptor (LDLr) which is down-regulated when intracellular cholesterol levels increase, while oxLDL is recognised by unregulated scavenger receptors, thus its uptake is the main driver of foam cell formation . Since numerous studies have demonstrated that nLDL may also directly contribute to foam cell formation [43–45], both nLDL and oxLDL were used in our studies.
The expression of the scavenger receptors CD36, CD68 and scavenger receptor-A (SR-A) has been shown to be upregulated in the presence of oxLDL and to a lesser extent nLDL [46–49], while LDLr expression is downregulated in response to cell exposure by nLDL [50, 51]. In the present work, the effects of nLDL and oxLDL on the expression of mRNA and protein for Myo6, Dab2, AP-2, and GIPC1 in THP-1 macrophages were investigated. Compared to control levels, nLDL significantly decreased mRNA transcript abundance for AP-2α2 and GIPC1 (Figures 8(c) and 8(d)), while incubation with oxLDL resulted in reduced levels of Myo6 and AP-2α2 mRNA (Figures 8(a) and 8(c)). Little change was seen at the protein level, however, except for a small decrease in Dab2 with nLDL (Figures 8(e)–8(h)). Both Myo6 protein and mRNA levels were significantly lower after incubation with oxLDL compared to nLDL (Figures 8(a) and 8(f)), suggesting that nLDL and oxLDL have different effects on the endocytic machinery, possibly reflecting their uptake via different receptor-mediated endocytic routes [52, 53].
We also examined the effects of knockingdown the expression of Myo6 and associated proteins on the uptake of nLDL and oxLDL. Although substantial knockdown of gene expression was achieved (Figure 9), we did not detect any significant effect on the uptake of lipoprotein type as assessed by fluorescence microscopy (Figure 10). These results, together with our findings of relatively small effects of the lipoproteins on mRNA and protein expression (Figure 8), suggest that Myo6 and its binding partners do not play a major role in the uptake of nLDL or oxLDL by macrophages during induction of foam cell formation.
The results presented here show that Myo6 and its associated proteins Dab2, AP-2, and GIPC are expressed in human macrophages, displaying similar patterns of expression and subcellular location in both the THP-1 cell line and in primary cells (HMDM). Myo6 was found to be particularly prominent in protrusions of the plasma membrane and membrane ruffles, where it was associated with F-actin. AP-2 and Dab2 appeared to be associated with cell vesicles, and AP-2, but not Myo6, was colocalised with Dab2. Although nLDL and oxLDL had some effects on the expression of the genes for the proteins investigated in macrophages, attenuation of their expression through the action of cognate siRNA molecules did not affect their uptake by the cells. Because the nature of these experiments requires large number of cells, however, HMDM could not be used, THP-1 cells being used instead; for this reason we remain cautious in extrapolating our findings to primary cells, as would be the case with any study involving immortalized cell lines. Nevertheless, the findings presented here on expression and subcellular localisation suggest that, in macrophages, Myo6 functions in cell adhesion and progression as well as in macropinocytosis. Data from the experiments on the uptake of LDL do not support the idea that it plays a major role in foam cell formation.
The authors of this paper do not have a direct financial relation with any commercial identity mentioned in this paper that might lead to a conflict of interests.
This work was supported by a Grant from the British Heart Foundation (FS/07/042) to Peter D. Chantler and Kathleen M. Botham.
- R. Albertini, R. Moratti, and G. De Luca, “Oxidation of low-density lipoprotein in atherosclerosis from basic biochemistry to clinical studies,” Current Molecular Medicine, vol. 2, no. 6, pp. 579–592, 2002.
- M. A. Hartman, D. Finan, S. Sivaramakrishnan, and J. A. Spudich, “Principles of unconventional Myosin function and targeting,” Annual Review of Cell and Developmental Biology, vol. 27, pp. 133–155, 2011.
- J. R. Sellers, “Myosins: a diverse superfamily,” Biochimica et Biophysica Acta, vol. 1496, no. 1, pp. 3–22, 2000.
- F. Odronitz and M. Kollmar, “Drawing the tree of eukaryotic life based on the analysis of 2,269 manually annotated myosins from 328 species,” Genome Biology, vol. 8, no. 9, article R196, 2007.
- A. L. Wells, A. W. Lin, L. Q. Chen et al., “Myosin VI is an actin-based motor that moves backwards,” Nature, vol. 401, no. 6752, pp. 505–508, 1999.
- F. Buss, S. D. Arden, M. Lindsay, J. P. Luzio, and J. Kendrick-Jones, “Myosin VI isoform localized to clathrin-coated vesicles with a role in clathrin-mediated endocytosis,” EMBO Journal, vol. 20, no. 14, pp. 3676–3684, 2001.
- F. Buss, G. Spudich, and J. Kendrick-Jones, “Myosin VI: cellular functions and motor properties,” Annual Review of Cell and Developmental Biology, vol. 20, pp. 649–676, 2004.
- T. Hasson, “Myosin VI: two distinct roles in endocytosis,” Journal of Cell Science, vol. 116, no. 17, pp. 3453–3461, 2003.
- F. Buss and J. Kendrick-Jones, “How are the cellular functions of myosin VI regulated within the cell?” Biochemical and Biophysical Research Communications, vol. 369, no. 1, pp. 165–175, 2008.
- S. D. Conner and S. L. Schmid, “Regulated portals of entry into the cell,” Nature, vol. 422, no. 6927, pp. 37–44, 2003.
- A. L. Dance, M. Miller, S. Seragaki et al., “Regulation of myosin-VI targeting to endocytic compartments,” Traffic, vol. 5, no. 10, pp. 798–813, 2004.
- G. J. Doherty and H. T. McMahon, “Mechanisms of endocytosis,” Annual Review of Biochemistry, vol. 78, pp. 857–902, 2009.
- F. Buss, J. Kendrick-Jones, C. Lionne, A. E. Knight, G. P. Côté, and J. P. Luzio, “The localization of myosin VI at the Golgi complex and leading edge of fibroblasts and its phosphorylation and recruitment into membrane ruffles of A431 cells after growth factor stimulation,” Journal of Cell Biology, vol. 143, no. 6, pp. 1535–1545, 1998.
- A. Inoue, O. Sato, K. Homma, and M. Ikebe, “DOC-2/DAB2 is the binding partner of myosin VI,” Biochemical and Biophysical Research Communications, vol. 292, no. 2, pp. 300–307, 2002.
- S. M. Morris, S. D. Arden, R. C. Roberts et al., “Myosin VI binds to and localises with Dab2, potentially linking receptor-mediated endocytosis and the actin cytoskeleton,” Traffic, vol. 3, no. 5, pp. 331–341, 2002.
- L. Aschenbrenner, T. T. Lee, and T. Hasson, “Myo6 facilitates the translocation of endocytic vesicles from cell peripheries,” Molecular Biology of the Cell, vol. 14, no. 7, pp. 2728–2743, 2003.
- J. P. Holt, K. Bottomly, and M. S. Mooseker, “Assessment of myosin II, Va, VI and VIIa loss of function on endocytosis and endocytic vesicle motility in bone marrow-derived dendritic cells,” Cell Motility and the Cytoskeleton, vol. 64, no. 10, pp. 756–766, 2007.
- J. V. Small, T. Stradal, E. Vignal, and K. Rottner, “The lamellipodium: where motility begins,” Trends in Cell Biology, vol. 12, no. 3, pp. 112–120, 2002.
- D. S. Reis, M. A. Souza, J. R. Mineo, and F. S. Espindola, “Myosin V and iNOS expression is enhanced in J774 murine macrophages treated with IFN-γ,” Brazilian Journal of Medical and Biological Research, vol. 34, no. 2, pp. 221–226, 2001.
- F. Rosenbauer, A. Kallies, M. Scheller et al., “Disabled-2 is transcriptionally regulated by ICSBP and augments macrophage spreading and adhesion,” EMBO Journal, vol. 21, no. 3, pp. 211–220, 2002.
- V. Braun, C. Deschamps, G. Raposo et al., “AP-1 and ARF1 control endosomal dynamics at sites of FcR-mediated phagocytosis,” Molecular Biology of the Cell, vol. 18, no. 12, pp. 4921–4931, 2007.
- S. S. Bohlson, M. Zhang, C. E. Ortiz, and A. J. Tenner, “CD93 interacts with the PDZ domain-containing adaptor protein GIPC: implications in the modulation of phagocytosis,” Journal of Leukocyte Biology, vol. 77, no. 1, pp. 80–89, 2005.
- T. T. Tuomisto, M. S. Riekkinen, H. Viita, A. L. Levonen, and S. Ylä-Herttuala, “Analysis of gene and protein expression during monocyte-macrophage differentiation and cholesterol loading-cDNA and protein array study,” Atherosclerosis, vol. 180, no. 2, pp. 283–291, 2005.
- Z. Qin, “The use of THP-1 cell as a model for mimicking the function and regulation of monocytes and macrophages in the vasculature,” Atherosclerosis, vol. 221, no. 1, pp. 2–11, 2012.
- J. V. Small, “Organization of actin in the leading edge of cultured cells: influence of osmium tetroxide and dehydration on the ultrastructure of actin meshworks,” Journal of Cell Biology, vol. 91, no. 3 I, pp. 695–705, 1981.
- M. H. Symons and T. J. Mitchison, “Control of actin polymerization in live and permeabilized fibroblasts,” Journal of Cell Biology, vol. 114, no. 3, pp. 503–513, 1991.
- L. P. Cramer and T. J. Mitchison, “Myosin is involved in postmitotic cell spreading,” Journal of Cell Biology, vol. 131, no. 1, pp. 179–189, 1995.
- U. P. Steinbrecher, S. Parthasarathy, and D. S. Leake, “Modification of low density lipoprotein by endothelial cells involves lipid peroxidation and degradation of low density lipoprotein phospholipids,” Proceedings of the National Academy of Sciences of the United States of America, vol. 81, no. 12, pp. 3883–3887, 1984.
- O. H. Lowry, N. J. Rosebrough, A. L. Farr, and R. J. Randall, “Protein measurement with the Folin phenol reagent,” The Journal of Biological Chemistry, vol. 193, no. 1, pp. 265–275, 1951.
- G. L. Peterson, “A simplification of the protein assay method of Lowry et al. Which is more generally applicable,” Analytical Biochemistry, vol. 83, no. 2, pp. 346–356, 1977.
- C. Puri, “Loss of myosin VI no insert isoform (NoI) induces a defect in clathrin-mediated endocytosis and leads to caveolar endocytosis of transferrin receptor,” Journal of Biological Chemistry, vol. 284, no. 50, pp. 34998–35014, 2009.
- X. X. Xu, W. Yang, S. Jackowski, and C. O. Rock, “Cloning of a novel phosphoprotein regulated by colony-stimulating factor 1 shares a domain with the Drosophila disabled gene product,” Journal of Biological Chemistry, vol. 270, no. 23, pp. 14184–14191, 1995.
- W. M. Bement, T. Hasson, J. A. Wirth, R. E. Cheney, and M. S. Mooseker, “Identification and overlapping expression of multiple unconventional myosin genes in vertebrate cell types,” Proceedings of the National Academy of Sciences of the United States of America, vol. 91, no. 14, pp. 6549–6553, 1994.
- H. Kirikoshi and M. Katoh, “Expression of human GIPC1 in normal tissues, cancer cell lines, and primary tumors,” International Journal of Molecular Medicine, vol. 9, no. 5, pp. 509–513, 2002.
- H. Yoshida, W. Cheng, J. Hung et al., “Lessons from border cell migration in the Drosophila ovary: a role for myosin VI in dissemination of human ovarian cancer,” Proceedings of the National Academy of Sciences of the United States of America, vol. 101, no. 21, pp. 8144–8149, 2004.
- M. V. Chibalina, C. Puri, J. Kendrick-Jones, and F. Buss, “Potential roles of myosin VI in cell motility,” Biochemical Society Transactions, vol. 37, no. 5, pp. 966–970, 2009.
- D. Valdembri, P. T. Caswell, K. I. Anderson et al., “Neuropilin-1/GIPC1 signaling regulates α5β1 integrin traffic and function in endothelial cells,” PLoS Biology, vol. 7, no. 1, Article ID e1000025, 2009.
- J. Z. Rappoport, “Focusing on clathrin-mediated endocytosis,” Biochemical Journal, vol. 412, no. 3, pp. 415–423, 2008.
- M. S. Robinson, “Adaptable adaptors for coated vesicles,” Trends in Cell Biology, vol. 14, no. 4, pp. 167–174, 2004.
- M. E. Maurer and J. A. Cooper, “The adaptor protein Dab2 sorts LDL receptors into coated pits independently of AP-2 and ARH,” Journal of Cell Science, vol. 119, no. 20, pp. 4235–4246, 2006.
- E. R. Eden, D. D. Patel, X. M. Sun et al., “Restoration of LDL receptor function in cells from patients with autosomal recessive hypercholesterolemia by retroviral expression of ARH1,” Journal of Clinical Investigation, vol. 110, no. 11, pp. 1695–1702, 2002.
- D. Chetrit, N. Ziv, and M. Ehrlich, “Dab2 regulates clathrin assembly and cell spreading,” Biochemical Journal, vol. 418, no. 3, pp. 701–715, 2009.
- H. S. Kruth, W. Huang, I. Ishii, and W. Y. Zhang, “Macrophage foam cell formation with native low density lipoprotein,” Journal of Biological Chemistry, vol. 277, no. 37, pp. 34573–34580, 2002.
- H. S. Kruth, N. L. Jones, W. Huang et al., “Macropinocytosis is the endocytic pathway that mediates macrophage foam cell formation with native low density lipoprotein,” Journal of Biological Chemistry, vol. 280, no. 3, pp. 2352–2360, 2005.
- X. Z. Ruan, Z. Varghese, S. H. Powis, and J. F. Moorhead, “Dysregulation of LDL receptor under the influence of inflammatory cytokines: a new pathway for foam cell formation,” Kidney International, vol. 60, no. 5, pp. 1716–1725, 2001.
- J. Han, D. P. Hajjar, M. Febbraio, and A. C. Nicholson, “Native and modified low density lipoproteins increase the functional expression of the macrophage class B scavenger receptor, CD36,” Journal of Biological Chemistry, vol. 272, no. 34, pp. 21654–21659, 1997.
- L. Nagy, P. Tontonoz, J. G. A. Alvarez, H. Chen, and R. M. Evans, “Oxidized LDL regulates macrophage gene expression through ligand activation of PPARγ,” Cell, vol. 93, no. 2, pp. 229–240, 1998.
- T. Nakagawa, S. Nozaki, M. Nishida et al., “Oxidized LDL increases and interferon-γ decreases expression of CD36 in human monocyte-derived macrophages,” Arteriosclerosis, Thrombosis, and Vascular Biology, vol. 18, no. 8, pp. 1350–1357, 1998.
- K. Tsukamoto, M. Kinoshita, K. Kojima et al., “Synergically increased expression of CD36, CLA-1 and CD68, but not of SR-A and LOX-1, with the progression to foam cells from macrophages,” Journal of Atherosclerosis and Thrombosis, vol. 9, no. 1, pp. 57–64, 2002.
- J. R. Smith, T. F. Osborne, J. L. Goldstein, and M. S. Brown, “Identification of nucleotides responsible for enhancer activity of sterol regulatory element in low density lipoprotein receptor gene,” Journal of Biological Chemistry, vol. 265, no. 4, pp. 2306–2310, 1990.
- D. Steinberg, “Low density lipoprotein oxidation and its pathobiological significance,” Journal of Biological Chemistry, vol. 272, no. 34, pp. 20963–20966, 1997.
- V. V. Kunjathoor, M. Febbraio, E. A. Podrez et al., “Scavenger receptors class A-I/II and CD36 are the principal receptors responsible for the uptake of modified low density lipoprotein leading to lipid loading in macrophages,” Journal of Biological Chemistry, vol. 277, no. 51, pp. 49982–49988, 2002.
- Y. Zeng, N. Tao, K. N. Chung, J. E. Heuser, and D. M. Lublin, “Endocytosis of oxidized low density lipoprotein through scavenger receptor CD36 utilizes a lipid raft pathway that does not require caveolin-1,” Journal of Biological Chemistry, vol. 278, no. 46, pp. 45931–45936, 2003.