Monocyte Chemotactic Protein-1 Regulates Voltage-Gated K+ Channels and Macrophage Transmigration
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- Gendelman, H.E., Ding, S., Gong, N. et al. J Neuroimmune Pharmacol (2009) 4: 47. doi:10.1007/s11481-008-9135-1
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Progressive human immunodeficiency virus (HIV)-1 infection and virus-induced neuroinflammatory responses effectuate monocyte-macrophage transmigration across the blood–brain barrier (BBB). A key factor in mediating these events is monocyte chemotactic protein-1 (MCP-1). Upregulated glial-derived MCP-1 in HIV-1-infected brain tissues generates a gradient for monocyte recruitment into the nervous system. We posit that the inter-relationships between MCP-1, voltage-gated ion channels, cell shape and volume, and cell mobility underlie monocyte transmigration across the BBB. In this regard, MCP-1 serves both as a chemoattractant and an inducer of monocyte-macrophage ion flux affecting cell shape and mobility. To address this hypothesis, MCP-1-treated bone marrow-derived macrophages (BMM) were analyzed for gene and protein expression, electrophysiology, and capacity to migrate across a laboratory constructed BBB. MCP-1 enhanced K+ channel gene (KCNA3) and channel protein expression. Electrophysiological studies revealed that MCP-1 increased outward K+ currents in a dose-dependent manner. In vitro studies demonstrated that MCP-1 increased BMM migration across an artificial BBB, and the MCP-1-induced BMM migration was blocked by tetraethylammonium, a voltage-gated K+ channel blocker. Together these data demonstrated that MCP-1 affects macrophage migratory movement through regulation of voltage-gated K+ channels and, as such, provides a novel therapeutic strategy for neuroAIDS.
Keywordsmonocyte monocyte chemotactic protein-1 K+ channels blood–brain barrier
Chemokines are structurally defined small proteins that serve as leukocyte chemoattractants for a variety of inflammatory diseases including those of the central nervous system (CNS; Rebenko-Moll et al. 2006; Callewaere et al. 2007; Mines et al. 2007). They affect a variety of divergent biological activities that include cell migration to sites of disease and inflammation, leukocyte activation, leukocyte secretions, and microbial activities (infection and cellular clearance; Callahan and Ransohoff 2004; Banisadr et al. 2005; Rebenko-Moll et al. 2006; Ubogu et al. 2006; Li and Ransohoff 2008). One of the most investigated and disease-associated chemokine is monocyte chemoattractant protein-1 (MCP-1), which plays a pivotal role in the recruitment of mononuclear phagocytes (MP; blood-borne monocytes, dendritic cells, and macrophages) to sites of inflammation and malignancies (de la Rosa et al. 2003; Garlet et al. 2003; Yao et al. 2006; Buhling et al. 2007; Tsai et al. 2008). The mechanism of such recruitment is well studied. Indeed, migration of monocytes across the vascular endothelium is linked to cells tethering to the endothelium, rolling along the vascular surface, firmly adhering to the endothelium, and finally diapedesis between tight morphologically structured endothelial cells, processes that are explicatively linked to both chemokine and adhesion molecule expression (Strell et al. 2007; Vestweber 2007; Crane 2008). After penetration of the endothelial basement membrane, monocytes migrate through the extracellular matrix of the tissues where they differentiate into tissue macrophages and migrate to sites of inflammation (Whatling et al. 2004; Fulcher et al. 2006; Reinhart et al. 2006; Cesar et al. 2008). Monocyte migration is mediated through selectins and their ligands or integrins interacting with endothelial vascular cell adhesion molecule 1 (VCAM-1). VCAM-1 is expressed at low levels on the endothelium and upregulated after immune activation (Lane et al. 1996; Nottet et al. 1996). On the apical endothelial surface, the chemokines MCP-1 and macrophage inflammatory proteins-alpha/beta, (MIP-1alpha/beta) activate beta(2) integrins to facilitate firm adhesion (Biernacki et al. 2004; Maslin et al. 2005). Diapedesis by monocytes occurs through interaction between integrins on both the monocyte and the endothelial cells, followed by homophilic adhesion (Muller and Randolph 1999; Schenkel et al. 2002; Mamdouh et al. 2008). The intracellular mechanisms for these processes are linked to activation by tyrosine phosphorylation of cellular proteins and phosphorylation of the non-receptor tyrosine kinases Lyn, JAK2, the cytoskeletal binding protein paxillin, and downstream transcription factors STAT3 and STAT5 (Muller et al. 2005). In this manner, MCP-1 induces TNF-α and IL-1 production and promotes macrophage activation (Biswas and Sodhi 2002).
Monocyte trafficking is of special interest in studies of the neuropathogenesis of HIV infection, including establishment of viral reservoirs and the development of HIV-associated neurocognitive disorders (HAND; Venneti et al. 2004; Williams et al. 2005; Berman et al. 2006). However, the process of monocyte migration across the vascular endothelium and changes in migration that occur during HIV infection are incompletely understood. We theorized that since MCP-1 can elicit activation responses for macrophages, the actual influence of the chemokine on monocyte-macrophage physiology would be profound. In this manner, a linkage between MCP-1 and potassium (K+) channel expression would be apparent. Blockers of these channels altered the organization and structure of the cytoskeletal proteins actin, tubulin, and vimentin; adherence-mediated macrophage activation; and maintenance of cytoskeletal integrity and cell shape. Such cytoskeletal changes were associated with cell morphology changes. We now demonstrate that MCP-1 activation of monocytes leads to morphological alterations that are directly linked to K+ channels. Chemokine-mediated responses lead to a dosage escalation of channel responses and to alterations in size, shape, volume, and ingress across an artificial BBB. The observations, taken together, provide unique insights into how MCP-1 can affect movement of monocytes across barriers and most notably into the CNS.
Materials and methods
Bone marrow cells were obtained from femurs of 6-week-old C57/BL6 or BALB/c male mice (purchased from Jackson Laboratory, Bar Harbor, MN). Cells were cultured in Teflon flasks at 2 × 106 cells/ml in complete Dulbecco’s modified Eagle’s medium (DMEM) supplemented with 10% fetal bovine serum, 2 mM l-glutamine, and 1% penicillin/streptomycin) in the presence of mouse macrophage colony stimulating factor (M-CSF) 2 µg/ml (a gift from Wyeth, Cambridge, MA). After 5–6 days in culture, BMM were determined to be >95% CD11b+ by flow cytometry and utilized thereafter.
Whole-cell patch clamp recording
BMM were plated onto sterile glass coverslips at a density of 0.5 × 106 cells/slip. Whole-cell patch-clamp recordings were made using an Axopatch 200B amplifier (Molecular Devices, Sunnyvale, CA) interfaced with a Digidata 1322A digitizer (Molecular Devices) and controlled with pClamp Version 8.1 software (Molecular Devices). Whole-cell currents were filtered at 1 kHz, digitized at 10 kHz, and stored on a computer hard disk. Patch pipettes were fabricated from borosilicate glass capillaries using a Sutter P97 microelectrode puller, with tip resistances of 4–8 MΩ when filled with pipette solution containing (in mM) 130 K+ gluconate, 10 EGTA, 1 CaCl2, 1 MgCl2, and 10 HEPES (pH 7.2, 280 mOsm). The bathing solution contained (in mM) 135 Na + gluconate, 5 KCl, 1 CaCl2, 1 MgCl2, 10 HEPES, and 10 glucose (pH 7.4, 290 mOsm). Values of access resistance ranging from 8 to 18 MΩ were compensated at 60–70% in most cells. Whole-cell voltage-dependent outward K+ currents were recorded in response to a series of voltage steps from −160 to +100 mV in 20 mV increments, starting from a holding potential of −60 mV. The steady-state current magnitudes were measured and normalized as a percentage of the magnitudes generated by a voltage step from −60 mV to +100 mV in control (perfused with normal bath solution). For statistical analyses, paired Student’s t tests were used with statistical significance at p < 0.05.
Isolation and culture of primary human monocytes
Human monocytes were obtained from HIV-1, HIV-2, and hepatitis B seronegative adults by leukophoresis and purified by countercurrent centrifugal elutriation. Monocytes were cultured in DMEM (Sigma, St. Louis) supplemented with 10% heat-inactivated human serum, 2 mM l-glutamine, gentamicin (50 μg/ml), and 2 μg/ml M-CSF. After 7 days in culture, monocytes differentiated into macrophages and the monocyte-derived macrophages (MDM) were infected with HIV-1ADA at a multiplicity of infection of 0.01 for 24 h before being injected into the brain of severe combined immunodeficient (SCID) mice.
SCID mouse model of HIVE
SCID mice (male C.B-17, 4 weeks old) were purchased from the Charles River Laboratories (Wilmington, MA). Each animal was inoculated in the basal ganglia (caudate and putamen) with 5 μl of either an HIV-1ADA-infected or uninfected human MDM suspension containing 3 × 105 cells. All animal procedures were approved by the Institutional Animal Care and Use Committee of University of Nebraska Medical Center.
BMM tracking by CT/SPECT
BMM were labeled with 111indium (111In) oxyquinoline (Indium oxine, GE Healthcare, Arlington Heights, IL) at a dose of 600 μCi per 30 × 106 cells in 1 ml RPMI 1640 supplemented with 10 mM HEPES for 45 min at 37°C. Cells were washed and resuspended in Hank’s buffered salt solution. Labeling efficiency was determined by γ-scintillation spectrometry (Packard Instrument Co., Meriden, CT) and was >75% of total input isotope. Each recipient mouse received 111In-labeled BMM by i.v. injection. Replicate groups of animals were simultaneously injected intraperitoneally (i.p.) with 4-aminopyridine daily (4-AP, 1 mg/kg) dissolved in phosphate-buffered saline (PBS). Mice were anesthetized with 0.5–1% isoflurane delivered in a 2:1 mixture of nitrous oxide and oxygen. Image acquisition was accomplished by a computed tomography/single photon emission computed tomography system (CT/SPECT; FLEX Triumph, Gamma Medica-Ideas, Northridge, CA). CT images were acquired by an X-ray detector, while SPECT images were acquired with a γ-scintillation camera detector fitted with 5 pinhole collimator. Co-registration of anatomical CT images and functional SPECT was performed by 3D image visualization and analysis software VIVID Gamma Medica-Ideas). The specific tissue and region of interest (ROI) of active viral encephalitis were defined and relative radioactivity for each area determined.
RNA extraction and real-time RT-PCR
Total RNA was isolated from cells using TRIzol Reagent (Invitrogen, Carlsbad, CA) and was purified by RNeasy Mini Kit (Qiagen, Inc., Valencia, CA). Real-time reverse transcription polymerase chain reaction (RT-PCR) for mouse KCNA3, KCND1, and KCNN4 was performed using the one-step quantitative TaqMan real-time RT-PCR system (Applied Biosystems, Inc., Foster City, CA). Gene expression levels were normalized to glyceraldehyde 3-phosphate dehydrogenase (GAPDH) as internal control.
Total proteins were prepared from BMM treated with MCP-1 or lipopolysaccharide (LPS) and equivalent amounts were electrophoretically separated on 4–15% sodium dodecyl sulfate polyacrylamide gel then transferred to Trans-Blot nitrocellulose membrane (BioRad, Hercules, CA). The membranes were probed with rabbit polyclonal antibodies to Kv1.3 and Kv1.5 (Almonade Lab, Israel) and images visualized with a chemoilluminescent horseradish peroxidase substrate kit (Pierce Biotechnology, Rockford, IL).
BMM were fixed in 3.7% formaldehyde solution for 10 min at room temperature, permeabilized in 0.1% Triton X-100 for 3 to 5 min. Nonspecific binding on BMM was blocked with 1% bovine serum albumin in phosphate-buffered saline for 30 min and stained for actin expression with rhodamine phalloidin. All samples were viewed on a confocal microscope.
BMM were labeled with 2.5 μM 5-chloromethylfluorescein diacetate (CMFDA) (Invitrogen) in serum-free DMEM at 37°C for 15 min, washed, and adjusted to 3 × 106 cells/ml in complete DMEM. Tetraethylammonium chloride (TEA) was used to inhibit K+ channels. The CMFDA-labeled cells were loaded into chemotaxis µ-slides (ibidi, GmbH, Munich, Germany) in 10 μl per chamber and incubated at 37°C for 35 min to allow cell attachment. Fresh or conditioned media (CM) was loaded into adjacent reservoirs of central channel, and the cells were imaged continuously for 2 h using a Nikon swept-field laser confocal microscope (Nikon Instruments, New York, NY). Images were analyzed using different plugins interfaced with ImageJ 1.38X software (Rasband, W.S., ImageJ, US National Institutes of Health, Bethesda, MD, USA, http://rsb.info.nih.gov/ij/, 1997–2007). Migration coordination data for each observed cell was acquired with the Manual Tracking plugin (Fabrice Cordelières, Institut Curie, Orsay, France). Chemotaxis plots and migration velocities of each cell were determined with the Chemotaxis and Migration Tool (ibidi).
Transendothelial migration of BMM assay was measured using a quantitative fluorescence-based assay. First, mouse brain endothelial cells b.END3 (ATCC, Manassas, VA) were plated on rat-tail collagen type-I-coated FluoroBlok tinted tissue culture inserts (with 3-μm pores; BD Biosciences, San Diego, CA) at a density of 1.5 × 104 cells/insert (Ramirez et al. 2008; Yamamoto et al. 2008). Thereafter, endothelial cells and BMM were treated with TEA for 30 min, and recombinant mouse MCP-1 (CCL2/MCP-1, 30 ng/ml; R&D Systems, Minneapolis, MN) was introduced into the lower chamber to create a chemokine gradient similar to that present in neuroinflammatory disorders. Labeled BMM (8 × 104 cells/insert loaded with calcein-AM at 5 μM/1 × 106 cells for 45 min) were placed in the upper chamber, and migration was allowed to continue up to 4 h at 37°C. Migration was monitored by measuring the relative fluorescence of the labeled BMM found in the lower chamber by fluorescence spectrometry (Molecular Devices). The numbers of migrated BMM were derived from a standard curve of the relative fluorescence as a function of known numbers of labeled BMM.
MCP-1 increased outward K+ currents in BMM
MCP-1 regulates K+ channel gene expression
MCP-1 affects BMM F-actin reorganization
MCP-1 facilitated BMM migration and is blocked by K+ channel antagonists
K+ channels regulate BMM BBB transmigration
CT/SPECT analysis of 111In-labeled BMM transmigration in peripheral tissues
CT/SPECT analysis of 111In-labeled BMM transmigration into brains of HIVE mice
Several different subtypes of Kv channels are expressed in human and mouse monocytes and macrophages including, but not limited to Kv1.3, Kv1.5 (Gallin 1991; Mackenzie et al. 2003; Vicente et al. 2003). These channels play an important role in controlling macrophage functions such as proliferation, activation, migration, and cytokine production (Gallin 1991; DeCoursey et al. 1996; Qiu et al. 2002). Studies have shown that Kv channels in macrophages can be regulated by many factors including proinflammatory cytokines. In the present study, we have demonstrated that MCP-1, a glial-derived cytokine, enhanced outward K+ currents and macrophage transmigration via regulation of Kv channel expression and channel activity. Our results herein fully support works by others demonstrating the expression of Kv channels in monocytes and macrophages (Mackenzie et al. 2003; Vicente et al. 2005, 2006; Irvine et al. 2007; Villalonga et al. 2007). Voltage-gated K+ channels including Kv1.3 channels are operative in blood-borne macrophages, tissue macrophages, and microglia, and are prominently induced concomitant with M-CSF-dependent proliferation.
It is well known that differential channel regulation affects intracellular signals and is linked to macrophage activation and differentiation as well as to immune, morphological, and migratory responses of the cells (DeCoursey et al. 1996; Mackenzie et al. 2003; Fordyce et al. 2005; Rus et al. 2005; Vicente et al. 2005; Irvine et al. 2007). LPS activation, for example, differentially regulates channel expression, as demonstrated by the induction of Kv1.3 channels and down-regulation of Kir2.1 channels. This modulation is dependent on the mode of macrophage immune responses (Gerth et al. 2005; Lei et al. 2005; Hoa et al. 2007; Villalonga et al. 2007). In this report, we have shown by pharmacological, mRNA, and protein analyses that macrophage ion currents are operative through Kv1.3 and Kir2.1 channels. This provides further support for the physiological importance of potassium channels in macrophage immunity. For example, it is well known that Kv1.3 channels are those principally found in macrophages and in other blood leukocytes (Mackenzie et al. 2003; Vicente et al. 2003; Fordyce et al. 2005; Vicente et al. 2005). For T cells, these channels are important since they serve as a primary regulator and affector of cell activation, as well as in maintaining resting membrane potential and ion homeostasis (Estes et al. 2008; Poulopoulou et al. 2008). Importantly, less is known about the functional roles of channels in disease, although Kv1.3 blockade has been shown to reduce proinflammatory cytokine secretion and cell proliferation (Irvine et al. 2007), as well as to slow cell movement. Such findings serve as a foundation for investigations into whether channel modulation can be utilized as a therapeutic target for autoimmune disease such as multiple sclerosis as suggested from studies showing that selective Kv1.3 channel blockers diminish disease progression in experimental allergic encephalomyelitis (Gonsette 2004; Vianna-Jorge and Suarez-Kurtz 2004; Beeton and Chandy 2005; Panyi 2005; Rus et al. 2005; Beraud et al. 2006).
In hippocampal microglia, Kv channel toxins affect pathobiological responses and cell migration across tissue barriers (Bordey and Spencer 2003; Fordyce et al. 2005; Thomas et al. 2007). Cytokines, toll receptor activation, and phorbol esters upregulate macrophage expression of Kv channels. Kv channel expression has been shown to be strongly upregulated in macrophage populations and only recently has the functional role of these channels been shown. First, extracellular K+ can activate T cell ß1 integrin and mediate adhesion and cell migration (Levite et al. 2000; Artym and Petty 2002; Davis et al. 2002). The gating of leukocyte voltage-gated K+ channels (Kv1.3) affects physiological responses, including elevated extracellular K+ levels, integrin functions, and cell volume changes since they are linked to cell migration (Colden-Stanfield and Scanlon 2000; Colden-Stanfield 2002). Ion channels are known to affect macrophage function. For human macrophages, the major ionic currents are carried by an outwardly rectifying K+ channel activated by adhesion onto a substrate stretch applied to membrane patches. While K+ channels govern properties of cell movement, chloride and K+ channels contribute to the regulation of biological responses including nitric oxide. Indeed, nitric oxide synthase is inhibited by channel blockers. Thus, a range of ion channels expressed by macrophages and microglia is linked to cell biology (Gerth et al. 2005; Lei et al. 2005; Hoa et al. 2007; Villalonga et al. 2007).
The linkages shown in this report between MCP-1, K+ channels, and macrophage migration across the BBB are significant in regards to the pathogenesis of HAND for a variety of reasons. HIV-1 transactivator protein Tat or progeny virus released from infected macrophages significantly increases astrocyte production and release of MCP-1 (Eugenin et al. 2005; El-Hage et al. 2006). MCP-1 is also expressed at high levels in the brains of patients with HIV-1-associated dementia (HAD), and MCP-1 levels within the cerebrospinal fluid correlate with the severity of neurological dysfunction (Sevigny et al. 2004; Maslin et al. 2005; Sevigny et al. 2007). Such observations are mirrored in simian immunodeficiency virus infected macaques with pathological features of HIVE (Zink and Clements 2002; Mankowski et al. 2004; Harrington et al. 2007). Homozygosity for the MCP-1-2578G allele was linked to a 50% reduction in the risk of HIV-1 acquisition. However, following HIV-1 infection, this MCP-1 genotype was associated with accelerated disease and a 4.5-fold increased risk of acquiring HAD. The mutant MCP-1-2578G allele yields increased transcriptional activity, protein production, and serum MCP-1 levels concomitant with accelerated MP tissue migration (Gonzalez et al. 2002).
To evaluate the biological significance of potassium channel influence on BMM migration into the brain, we investigated BMM migration in a SCID mouse model with HIVE using CT/SPECT. HIVE was induced by i.c. injection of HIV-1ADA-infected MDM into the caudate and putamen of SCID mice and was characterized by robust inflammation and the generation of an MCP-1 gradient for BMM attraction into sites of active disease. In this work, comparisons of BMM brain migration between uninfected and HIVE mice that were either untreated or treated with 4-aminopyridine (4-AP), a K+ channel blocker, showed that Kv channel blocker had no effects on BMM distribution in the peripheral organs but significantly reduced BMM migration into the mouse brain. These results further reinforce the biological importance of potassium channels for macrophage migration and its links to MCP-1 and inflammatory responses.
The data, taken together, build on previous works demonstrating a link between MCP-1 induced biological responses and specific ion channels. MCP-1 certainly has a multifaceted role in HAND through its abilities to affect proinflammatory properties and contribute to disease progression and increased risk of dementia by affecting MP ingress into the brain. The importance of the current study rests in that these physiological responses to MCP-1 play a central role in HAND and as such opens up new therapeutic targets for disease.
The authors thank Mr. Anil Papugani for his help in BMM migration across murine blood–brain barrier experiments. The authors extend their thanks to Robin Taylor for her critical reading of the manuscript. The work was supported by the Frances and Louis Blumkin Foundation, the Community Neuroscience Pride of Nebraska Initiative, the Carol Swartz, M.D. Emerging Neuroscience Laboratory, and the Alan Baer Charitable Trust (to H.E.G.), NIH grants P01 NS31492 (to D.J.V.), R01 MH65151 (to Y.P.), R01 NS041862 (to H.X.), 2R37 NS36126, P01 NS043985, and P20 RR15635 (to H.E.G.).
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