Cytosolic phospholipase A2 plays a crucial role in ROS/NO signaling during microglial activation through the lipoxygenase pathway
© Chuang et al. 2015
Received: 23 August 2015
Accepted: 21 October 2015
Published: 31 October 2015
Oxidative stress and inflammation are important factors contributing to the pathophysiology of numerous neurological disorders, including Alzheimer’s disease, Parkinson’s disease, acute stroke, and infections of the brain. There is well-established evidence that proinflammatory cytokines and glutamate, as well as reactive oxygen species (ROS) and nitric oxide (NO), are produced upon microglia activation, and these are important factors contributing to inflammatory responses and cytotoxic damage to surrounding neurons and neighboring cells. Microglial cells express relatively high levels of cytosolic phospholipase A2 (cPLA2), an enzyme known to regulate membrane phospholipid homeostasis and release of arachidonic acid (AA) for synthesis of eicosanoids. The goal for this study is to elucidate the role of cPLA2IV in mediating the oxidative and inflammatory responses in microglial cells.
Experiments involved primary microglia cells isolated from transgenic mice deficient in cPLA2α or iPLA2β, as well as murine immortalized BV-2 microglial cells. Inhibitors of cPLA2/iPLA2/cyclooxygenase (COX)/lipoxygenase (LOX) were used in BV-2 microglial cell line. siRNA transfection was employed to knockdown cPLA2 expression in BV-2 cells. Griess reaction protocol was used to determine NO concentration, and CM-H2DCF-DA was used to detect ROS production in primary microglia and BV-2 cells. WST-1 assay was used to assess cell viability. Western blotting was used to assess protein expression levels. Immunocytochemical staining for phalloidin against F-actin was used to demonstrate cell morphology.
In both primary and BV-2 microglial cells, stimulation with lipopolysaccharide (LPS) or interferon gamma (IFNγ) resulted in a time-dependent increase in phosphorylation of cPLA2 together with ERK1/2. In BV-2 cells, LPS- and IFNγ-induced ROS and NO production was inhibited by arachidonyl trifluoromethyl ketone (AACOCF3) and pyrrophenone as well as RNA interference, but not BEL, suggesting a link between cPLA2, and not iPLA2, on LPS/IFNγ-induced nitrosative and oxidative stress in microglial cells. Primary microglial cells isolated from cPLA2α-deficient mice generated significantly less NO and ROS as compared with the wild-type mice. Microglia isolated from iPLA2β-deficient mice did not show a decrease in LPS-induced NO and ROS production. LPS/IFNγ induced morphological changes in primary microglia, and these changes were mitigated by AACOCF3. Interestingly, despite that LPS and IFNγ induced an increase in phospho-cPLA2 and prostaglandin E2 (PGE2) release, LPS- and IFNγ-induced NO and ROS production were not altered by the COX-1/2 inhibitor but were suppressed by the LOX-12 and LOX-15 inhibitors instead.
In summary, the results in this study demonstrated the role of cPLA2 in microglial activation with metabolic links to oxidative and inflammatory responses, and this was in part regulated by the AA metabolic pathways, namely the LOXs. Further studies with targeted inhibition of cPLA2/LOX in microglia during neuroinflammatory conditions can be valuable to investigate the therapeutic potential in ameliorating neurological disease pathology.
KeywordsMicroglia cPLA2 Arachidonic acid Lipoxygenase ROS NO
Neuroinflammation plays a major role in the progression of neurodegenerative diseases including Alzheimer’s disease, Parkinson’s diseases, cerebral vascular stroke, and infectious HIV encephalopathy. Microglial cells, the resident innate immune cells in the central nervous system (CNS), are known to exert multiple physiologic functions in the brain, including anchoring CNS innate immune response through phagocytosis of foreign pathogens, removing cellular breakdown products, stimulating tissue repair process, and maintaining tissue homeostasis . Activation of microglial cells can also exert significant impact on the propagation of inflammatory responses [2, 3]. For instance, activated microglia was shown in vivo to contribute to expansion of infarct after focal cerebral ischemia , and inhibition of microglial activation was proven a viable strategy to prevent inflammatory neuronal death in vitro . Recent studies had place much focus on the differential functions of polarized M1/M2 microglial cells after activation. While much research is currently underway to distinguish the biochemical and functional properties of each phenotype, most tend to agree that M1 microglia are more cytotoxic and persist during the disease effector stage, whereas M2 microglia are more neuroprotective and predominate during the repair stage [6–8]. The discovery of functional differences and delineation of time course of microglia polarization has generated interest in ways to limit M1 activation and stimulate M2 transformation in order to ameliorate outcomes of neurological diseases, including experimental stroke and traumatic brain injury [9–13].
Biochemically, M1 microglial activation is associated with the release of ROS, NO, glutamate, cytokines (such as TNFα), phospholipases, matrix metalloproteases, and other proinflammatory factors contributing to the progressive neuronal damage observed in many neurodegenerative disorders [14–16]. Therefore, suppressing or limiting microglial activation can have beneficial effects for preventing neuroinflammation and neurodegeneration. Microglia in vitro can be activated with a variety of agents, such as proinflammatory cytokines (TNFα, IL-1β, IFNγ), lipopolysaccharides (LPS), and oligomeric beta amyloid (Aβ) . Studies including those from our laboratory have demonstrated that microglia activation by proinflammatory cytokines and LPS causes induction of iNOS and activation of NADPH oxidase, leading to increased oxidative/nitrosative stress .
Phospholipase A2s (PLA2s) are groups of enzymes that hydrolyze the fatty acids from the sn-2 position of membrane phospholipids. Among the PLA2s identified, cPLA2 and iPLA2 are the constitutively active PLA2s that serve as important mediators for the release of polyunsaturated fatty acids, including arachidonic acid (AA) and docosahexaenoic acid from membrane phospholipids [19, 20]. Multiple studies have demonstrated group IV PLA2α (cPLA2α) to be the major PLA2 responsible for the release of AA and to play an essential role in inflammation. Transgenic mice lacking cPLA2α have been shown to display significantly reduced deleterious phenotypes in inflammatory diseases, such as ischemic brain injury, anaphylaxis, arthritis, alcoholism, and acute lung injury [21–27]. More recent in vivo studies demonstrated ability for pharmacological inhibitors of cPLA2 to ameliorate ischemic stroke, experimental autoimmune encephalitis, and spinal cord injury [28–30]. Although cPLA2 activation in the brain is associated with oxidative stress, neuronal excitation, and neuroinflammation , little is known about mechanism(s) for its activation in microglial cells . Previous studies demonstrated protective effects of cPLA2 inhibition against microglia-induced white matter damage in vivo and oligodendrocyte cell death in vitro, suggesting the role of this enzyme as a potential target to suppress microglia-induced secondary damage in the central nervous system . However, the mode of action of cPLA2 and its link to the inflammatory responses in microglial cells have not been elucidated in detail. In this study, we isolated primary microglial cells from cPLA2 and iPLA2 KO mice to demonstrate the role of cPLA2 (and not iPLA2) in mediating oxidative and inflammatory responses from LPS and IFNγ stimulation. In addition, we further suggested a mechanism that links cPLA2-mediated eicosanoid production with downstream ROS and NO generation in BV-2 microglial cells.
Dulbecco’s modified Eagle’s medium (DMEM), penicillin/streptomycin, and 0.25 % (w/v) trypsin/EDTA were obtained from GIBCO (Gaithersburg, MD). Endotoxin-free fetal bovine serum was from Atlanta Biologicals (Lawrenceville, GA). Lipopolysaccharide (LPS) (rough strains) from Escherichia coli F583 (Rd mutant) was purchased from Sigma-Aldrich (St. Louis, MO). Interferon-γ (IFNγ) was purchased from R&D Systems (Minneapolis, MN). Pharmacological inhibitors used include the following: U0126, SB202190, and SP600125 were from Cell Signaling (Beverly, MA). Arachidonyl trifluoromethyl ketone (AACOCF3), pyrrophenone, racemic bromoenol lactone (BEL), nordihydroguaiaretic acid (NDGA), ibuprofen, zileuton, and PD146176 were from Cayman Chemical (Ann Arbor, MI). NCTT-956 was from Sigma-Aldrich (St. Louis, MO). RNA interference Lipofectamine RNAiMAX Transfection Reagent was from Life Technology (Carlsbad, CA). siRNA against cPLA2 Mm_Pla2g4a_8 FlexiTube siRNA (NM_008869) and AllStars Negative Control siRNA were purchased from Qiagen (Hilden, Germany). Antibodies used for Western blots include the following: goat anti-rabbit IgG-horseradish peroxidase, goat anti-mouse IgG-horseradish peroxidase, anti-cPLA2 rabbit polyclonal, anti-iNOS rabbit polyclonal antibodies (Santa Cruz Biotechnology, Santa Cruz, CA); monoclonal anti-β-actin peroxidase (Sigma-Aldrich, St. Louis, MO); rabbit polyclonal anti-p-cPLA2, rabbit polyclonal anti-ERK1/2, and mouse monoclonal anti-phospho-ERK1/2 antibodies (Cell Signaling, Beverly, MA). An affinity-purified antibody directed against an iPLA2β peptide corresponding to residues 277–295 was a gift of Drs. Chris Jenkins and Richard Gross (Washington University School of Medicine, St. Louis, MO) . For immunocytochemical staining, rabbit anti-ionized calcium-binding adapter molecule 1 (Iba-1) antibodies (019–19741) was purchased from Wako BioProducts (Richmond, VA), Alexa Fluor 488® phalloidin from Life Technologies (Carlsbad, CA), and 4′,6-diamidino-2-phenylindole (DAPI) from Roche Molecular Chemicals (Basel, Switzerland). For ROS detection, CM-H2DCF-DA (DCF) was purchased from Invitrogen, Inc. (Eugene, OR). WST-1 assay was purchased from Clontech (Mountain View, CA). Prostaglandin E2 (PGE2) EIA Kit was purchased from Cayman Chemicals (Ann Arbor, MI).
cPLA2 transgenic animal breeding and genotyping
All animal care and experimental protocols were carried out in accordance with NIH guidelines and with permission from the University of Missouri Animal Care and Use Committee (protocol #6728). Pairs of C57Bl/6 male and female heterozygous cPLA2+/− mice were kindly provided by Dr Joseph V. Bonventre (Harvard Medical School, Boston, MA) and colony was expanded at the University of Missouri for more than five generations prior to start of the experiments. Wild-type cPLA2+/+ and homozygous knockout cPLA2−/− mice used in the experiments were generated by crossing male and female heterozygous cPLA2+/− mice, and genotyping of litters was done between postnatal day 3~6 by polymerase chain reaction (PCR) as previously described .
iPLA2 transgenic animal breeding and genotyping
iPLA2β-KO mice were housed and cared for in animal facilities administered through the Washington University Division of Comparative Medicine, and animal procedures were performed according to a protocol approved by the Washington University Animal Studies Committee. iPLA2β-KO mice were previously generated by insertion of the neomycin resistance gene into exon 9 of the mouse iPLA2β (Pla2g6) gene by homologous recombination [34, 35]. KO and WT mice were generated by mating heterozygous mice, and their genotype was determined by a PCR assay. The primers used for PCR genotyping were WT F1 (TTACCTCCGCTTCTCGTCCCTCATGGAGCT), Neo F1 (GGGAACTTCCTGACTAGGGGAGGAGTAGAA), and WT R1 (TCTGTTTCTCTAGAGACCCATGGGGCCTTG), which when combined in a single PCR reaction generate a 158-bp band for the WT allele and a 254-bp band for the KO allele.
Primary microglia isolation
Preparations of primary microglial cells with postnatal day 7–10 C57Bl/6 pups were accomplished with the Miltenyi Biotec MACS cell separation system (Bergisch Gladbach, Germany). Briefly, brains from the genotyped pups were dissected and meninges removed. Tissues were dissociated using the Neural Tissue Dissociation Kit (P) (Miltenyi Biotec) with the gentleMACS dissociator. Prior to isolation, cell concentration in the suspension was counted and roughly 105 cells were collected for flow cytometry analysis by the Cellular Immunology Core in the University of Missouri. Microglia were isolated from the single-cell suspension using the magnetic activated cell sorting (MACS) technology with anti-cluster of differentiation molecule 11b (CD11b) (Microglia) MicroBeads (Miltenyi Biotec) in combination with an OctoMACS Separator with slight modifications to the manufacturer’s instructions. The number of cells post-isolation was counted, and roughly 105 cells were collected for post-isolation flow cytometry analysis, and the remaining cells were plated at a density of 5 × 105/cm2. Plated cells were cultured in DMEM supplemented with 10 % FBS containing 100 units/mL penicillin and 100 μg/mL streptomycin and maintained in 5 % CO2 incubator at 37 °C. Culture medium was replaced every 3–5 days. Primary cell cultures were used between days-in-vitro (DIV)5–7.
Immortalized microglial BV-2 cell culture
The murine BV-2 cell line was generated by infecting primary microglia cell cultures with a v-raf/v-myc oncogene-carrying retrovirus (J2) . These cells were obtained as a gift from Dr. R. Donato  and prepared as previously described [18, 38]. Briefly, cells were cultured in DMEM (high glucose) supplemented with 10 % FBS containing 100 units/mL penicillin and 100 μg/mL streptomycin and maintained in 5 % CO2 incubator at 37 °C. For subculture, cells were removed from the culture flask by gentle scraping, re-suspended in the culture medium, and sub-cultured in 6/96-well plates for experiments. Cell condition and morphology were assessed by using a phase contrast Nikon DIAPHOT 300 microscope attached with a CCD cool camera, and MagnaFire2.1C software was used for image capture and processing. Representative bright field pictures were obtained using a 20× objective lens.
Flow cytometry for microglial cell purity analysis
During primary microglia isolation, after tissue dissociation and cell number were determined, roughly 105 cells were collected, resuspended in 100 μL buffer, and incubated with 10 μL CD11b-fluorescein isothiocyanate (FITC) antibodies (Miltenyi) for 10 min in 4 °C. Cells were then washed and resuspended in 100 μL fresh buffer for flow cytometry analysis. Similarly, after microglia isolating by CD11b cell sorting, 105 cells were collected and labeled with cd11b-FITC for flow cytometry analysis. Flow cytometry analysis was performed using the BD FACScan under the FITC protocol by the Cellular Immunology Core in the University of Missouri.
cPLA2 RNA interference knockdown in BV-2 cells
BV-2 cells were seeded in 96- and 24-well plates with antibiotic-free DMEM containing 5 % FBS for 24 h. When cell density reached roughly 70–80 %, they were transfected with either AllStars negative control siRNA (Qiagen) or cPLA2 siRNA (NM_008869, Qiagen) (final concentration of 40 nM) using the RNAiMAX transfection reagent (Invitrogen) in mixture of Opti-MEM and DMEM mediums for 48 h prior to being used for experiments, according to the manufacturer’s instructions. cPLA2 knockdown was evaluated by Western blot for protein expression of total cPLA2 normalized against β-actin.
Cell viability assay protocol
The WST-1 protocol was used for assessment of cell viability. Briefly, after reaching 80–90 % confluence, cells in 96-well plates were serum starved for 4 h, followed by incubation with inhibitors for 16 h. After treatment, cell viability was determined by adding 10 μL of the WST-1 reagent (Roche Applied Science, Germany) into each well. After gentle shaking, cells were incubated for 1 h at 37 °C and absorbance was read at 450 nm (with reference wavelength at 650 nm).
NO released from BV-2 cells was converted to nitrite in the culture medium. NO concentration was measured using the Griess reagent protocol as described previously . In brief, BV-2 cells in 96-well plate were serum starved in phenol red-free DMEM for 3 h, followed by incubation with designated inhibitors for 1 h. Cell were then incubated with IFNγ or LPS at 37 °C for 16 h. Alternatively, primary microglia were stimulated with IFNγ or LPS at 37 °C for 24/48 h. Aliquots of medium (50 μL) were incubated with 50 μL of the reagent A [1 % (w/v) sulfanilamide in 5 % phosphoric acid, Sigma-Aldrich] for 10 min at room temperature covered in dark. This was followed by addition of 50 μL of reagent B [0.1 %, w/v, N-1-naphthylethylenediamine dihydrochloride, Sigma-Aldrich] for 10 min at room temperature, protected from light, and absorbance at 543 nm was measured using a microplate reader (Biotek Synergy 4, Winooski, VT). Serial dilutions of sodium nitrite (0–100 μM) were used to generate the nitrite standard curve.
ROS production in microglial cells was assessed with 5-(and-6)-chloromethyl-2′,7′-dichlorodihydrofluorescein diacetate (CM-H2DCF-DA, or DCF in short). Primary microglia or BV-2 microglial cells were seeded in 96-well plate and grown until 90 % confluent. Cells were serum starved for 3 h, followed by pretreatment with inhibitors for 1 h, prior to stimulation with LPS or IFNγ for 11 h. Alternatively, primary microglia were stimulated with IFNγ or LPS at 37 °C for 24/48 h. DCF (10 μM) was added to each well and incubated for 1 h. The fluorescent intensity of DCF was measured with a microplate reader (excitation wavelength of 490 nm and emission wavelength of 520 nm). Fluorescent intensity was normalized against control wells for statistical analysis.
PGE2 ELISA protocol
PGE2 concentration in the cell-conditioned medium was assessed with the PGE2 ELISA protocol (Cayman Chemicals). Briefly, 50 μL of conditioned medium from treated BV-2 cells in 96-well plates were incubated with 50 μL of PGE2 monoclonal antibody and 50 μL of PGE2 AChE tracer for 18 h at 4 °C with plate covered with plastic film. Standard curve was generated with serial dilution of PGE2 EIA standard (Cayman No. 414014) in EIA buffer prepared according to Cayman’s protocol. On day 2, 100 dtn of Ellman’s Reagent was reconstituted with 20 mL of UltraPure water and 200 μL added into each sample/standard well for development. The plate was placed on an orbital shaker for 60 min prior to measuring for absorbance at 410 nm using a microplate reader. Concentration was calculated from the fourth-degree polynomial curve generated from the standard wells in accordance to kit instruction.
Western blot analysis
Cell lysates were collected in RIPA buffer containing 50 mM Tris–HCl (pH 7.5), 150 mM NaCl, 1 % Nonidet P-40, and 0.1 % SDS. The extract was centrifuged at 10,000×g for 15 min at 4 °C and transferred to a clean tube to remove cell debris. Protein concentration was measured and normalized with the BCA protein assay kit (Pierce Biotechnology, Rockford, IL). Depending on the target of interest, 5–10 μg of total protein was loaded in SDS-PAGE for electrophoresis. After electrophoresis, proteins were transferred to 0.45-μm nitrocellulose membranes. Membranes were incubated in Tris-buffered saline containing 0.1 % Tween 20 (TBS-T) and 5 % non-fat milk for 1 h at room temperature. The blots were incubated at 4 °C overnight with antibodies cPLA2 (1:1000), phospho-cPLA2 (1:1000), ERK1/2 (1:2000), phospho-ERK1/2 (1:1000), iNOS polyclonal (1:1000), and β-actin (1:50,000). After repeated washing with 1X TBS-T, blots were incubated with goat anti-rabbit IgG-HRP (1:4000) or goat anti-mouse IgG-HRP (1:2000) for 1 h at room temperature. Immunolabeling was detected by chemiluminescence ECL/WestPico/Femto and developed in X-ray film developer. Films were scanned, and the optical density of bands was measured with the QuantityOne software (BioRad, Hercules, CA).
Immunocytochemistry staining was carried out as previously described by Chuang et al. . Briefly, cells were cultured in 24-well plates containing round cover slips. After treatment, cells were fixed in 4 % paraformaldehyde for 15 min and then permeabilized with 0.1 % Triton X-100 in PBS for 30 min. Cells were incubated with 10 % normal goat serum in 0.005 % Triton X-100 in PBS for 60 min then incubated overnight in 0.5 % normal goat serum in 0.005 % Triton X-100 in PBS containing primary antibodies. The next day, cells were incubated in 0.005 % Triton X-100 in PBS containing secondary antibodies, goat-anti-rabbit Alexa fluor 488 (Jackson Immunoresearch), and goat-anti-mouse Alexa fluor 549 (Jackson Immunoresearch) for 60 min, followed by 1 unit of Alexa Fluor 488 phalloidin (Life Technologies)/well for 20 min (5 μL of 6.6 μM stock solution dissolved in methanol diluted in 200 μL of 0.005 % Triton X-100 in PBS), and nuclear counterstaining with 1 μg/mL of 4,6-diamidine-2-phenylindole dihydrochloride (DAPI) (Pierce) in PBS for 10 min. The coverslips were then mounted on fluoromount (Sigma-Aldrich) and sealed with nail polish. Fluorescence photomicrographs were captured using a Leica DMI 6000B fully automated epifluorescence microscope (Leica Microsystems Inc., Buffalo Grove, IL).
Data were presented as means ± SEM. Results were analyzed either by one-way ANOVA followed by Dunnett’s multiple comparison tests (V4.00; GraphPad Prism Software Inc., San Diego, CA). Statistical significance was considered for P < 0.05.
Stimulation of iNOS, p-ERK1/2, and p-cPLA2 protein expression by LPS and IFNγ in primary and immortalized (BV-2) microglial cells
cPLA2 phosphorylation is regulated by phospho-ERK1/2
LPS- and IFNγ-induced iNOS expression and NO production are significantly decreased in microglia deficient in cPLA2
LPS- and IFNγ-induced ROS from WT and cPLA2 KO microglia
Pharmacological inhibition and siRNA of cPLA2 result in suppression of LPS- and IFNγ-induced NO production in BV-2 cells
RNA interference was further employed to ensure the inhibition observed above was not resulted from non-specific pharmacological effects. Using the cPLA2 siRNA (NM_008869, Qiagen) and RNAiMAX transfection reagent, we were able to knockdown cPLA2 by 70–80 %, based on protein expression by Western blot (Additional file 2: Figure S2). Under this condition, NO production was significantly suppressed in knockdown cultures as compared with control cultures (Fig. 6e, f).
Pharmacological inhibition and siRNA of cPLA2 result in significant suppression of LPS- and IFNγ-induced ROS production in BV-2 cells
cPLA2 inhibition prevents morphological changes associated with activation in primary microglia
Ca2+-independent PLA2 does not alter LPS- and IFNγ-induced iNOS/NO/ROS production
To further verify the results, we also tested whether selective iPLA2 inhibitor BEL (racemic) may have an effect on LPS- and IFNγ-induced NO and ROS production in BV-2 cells. As shown in Fig. 9d–g, results indicated that BEL did not significantly affect the amount of NO or ROS produced by either stimulus.
cPLA2-dependent induction of NO or ROS in microglia does not go through COX-1/2
LOX inhibition significantly suppresses cPLA2-dependent microglial induction of ROS and NO
cPLA2 plays a significant role in microglial activation
cPLA2 has been shown to play a significant role in mediating oxidative/nitrosative and inflammatory responses in neurons, astrocytes, and other cells [46, 47], but less attention has been paid to microglia. The findings of this study clearly demonstrate the involvement of cPLA2 in LPS- and IFNγ-induced ROS and NO production in microglial cultures. To our knowledge, this is the first study to use primary microglia prepared from cPLA2 and iPLA2 knockout mice to provide new evidence for the significant role of cPLA2 in microglial activation.
The comparison between cPLA2 knockout and wild-type primary microglia cells showed that cPLA2 not only plays a crucial role in activating the oxidative/inflammatory pathway, leading to generation and release of ROS/NO, but also to the overall morphological transformation of microglial cells after endotoxin/cytokine stimulation. To ensure that the findings are not a result of alternative mechanisms from long-term functional compensation in response to cPLA2 knockout, the same conclusion was reached using pharmacological inhibition, with AACOCF3 (non-specific) and pyrrophenone (specific), and RNA interference knockdown in BV-2 cells. Other studies using LPS but not IFNγ as a stimulator support this conclusion in rat primary microglia  and BV-2 cells . On the other hand, while iPLA2 is also constitutively expressed in microglia and a target of AACOCF3, results here with iPLA2 KO and pharmacological inhibition with BEL showed that this PLA2 has little role in mediating ROS and NO production in the BV-2 microglial cells. This result is in slight contrast to the prior study by Strokin et al., who suggested that iPLA2 also contributes to the proinflammatory responses in LPS-treated astrocytes via Ca2+ signaling . This difference may well be due to use of different cell type, i.e., microglia versus astrocytes.
The ERK1/2-cPLA2-ROS-iNOS axis in microglial activation
cPLA2 is known to have multiple active serine residues susceptible for phosphorylation. Among these serine residues, Ser505 was identified to be phosphorylated by MAPK and served as an important regulator for cPLA2 activity and subsequent AA release [32, 41]. In the study by Pavicevic with vascular smooth muscle cells, phosphorylation of Ser515 by CaMKII was shown to precede Ser505 phosphorylation and phosphorylation of both Ser515 and 505 sites is required for activation of this enzyme . In primary neurons in culture, stimulation with ionotropic glutamate receptor agonist such as NMDA resulted in ROS production through NADPH oxidase and rapid activation of ERK1/2 and cPLA2 . In this study, we demonstrated that LPS and IFNγ each mediated a time-dependent increase in phospho-ERK1/2 and cPLA2 in both primary and BV-2 microglial cells. In both conditions, the time for increase in p-ERK1/2 preceded that for p-cPLA2. The relationship between p-ERK1/2 and cPLA2 was further confirmed by U0126, the MEK1/2-ERK1/2 inhibitor, which readily abrogated phosphorylation of cPLA2.
NADPH oxidase in microglia cells has been shown to play a significant role in neurodegenerative diseases, such as alcohol-induced neurodegeneration , Alzheimer’s disease , and Parkinson’s disease . Previous study from our laboratory has demonstrated the production of ROS from NADPH oxidase to be upstream of NO production in BV-2 microglia cells. Our studies further demonstrated that in BV-2 microglial cells, LPS and IFNγ can individually stimulate ROS and iNOS/NO through phosphorylation of ERK1/2 [39, 40]. Study by Ribeiro et al. (2013) also demonstrated effects of cannabinoid receptor agonists and antagonists to suppress LPS-induced microglia activation via ERK1/2, cPLA2, and NF-κB. These results as well as ours placed LPS and IFNγ activation of ERK1/2 and cPLA2 upstream of the NF-κB transcriptional pathway. In rat microglial cells, Szaingurten-Solodkin observed a link between cPLA2 in NADPH oxidase and iNOS activated by aggregated Abeta1-42, a toxic peptide cleaved from the amyloid precursor protein . In their study, it was proposed that cPLA2 regulated NADPH oxidase activity, which in turn caused upregulation of cPLA2, COX-1/2, and iNOS through an NF-κB-dependent mechanism. Taken together, our results with cPLA2 inhibitors as well as siRNA knockdown well demonstrated the role of cPLA2 in mediating ROS and NO production upon stimulation by LPS and IFNγ. Our results with primary microglia isolated from cPLA2 KO brain further validated the link between cPLA2 on ROS and NO production in these cells.
Role of arachidonic acid and LOX in microglial activation
Earlier studies had linked cPLA2 or its downstream metabolites (i.e., AA or lysophospholipids) with ROS production from NADPH oxidase, although the exact mechanism remains to be investigated [55, 56]. In macrophages, there is evidence that cPLA2 can interact directly with NADPH oxidase subunits, namely p47phox and p67phox, which facilitate translocation of these subunits to membranes to form the active NADPH oxidase complex [55, 57]. Alternatively, downstream products of AA were proposed to be involved in ROS production from NADPH oxidase . Activation of cPLA2 and subsequent release of AA has been shown in the production of an array of eicosanoids, including the production of prostaglandins and leukotrienes through activation of COX and LOX. However, the extent for this action is cell dependent . A number of studies, including those from our own, have demonstrated the increase in PGE2 production upon stimulation with LPS and IFNγ in astroglial cells [59, 60]. In the present study with microglial cells, we showed that while the COX-1/2 inhibitor effectively inhibited LPS- and IFNγ-induced PGE2 production, this condition was not linked to the suppression of ROS and NO production by LPS and IFNγ.
While the action of COX-1/2 is well established in peripheral inflammation and a popular target for non-steroidal anti-inflammatory drugs (NSAIDs), its role in neuroinflammation is not well understood. Aspirin is used after acute stroke not for anti-inflammatory effect but rather for secondary prevention of atherosclerosis due to its antiplatelet properties through inhibition of prostaglandin and subsequent thromboxane A2 [61, 62]. Similarly, numerous recent large-scale double-blind placebo-controlled clinical trials have not found a beneficial effect of COX-1/2 inhibition in the treatment of neurological diseases where neuroinflammation is proposed to be involved, such as Alzheimer’s disease or depression [63, 64]. In agreement with our study, Minghetti and colleagues have also reported that microglial cell activation increased TNFα and COX-1/2, but this condition did not contribute to ROS/NO production [65, 66].
On the other hand, recent studies have generating growing recognition of LOX in mediating inflammation, and some have implicated its role in neuroinflammation. Lipoxygenases are known to mediate the pathophysiology of numerous inflammatory diseases, including asthma, immune disorders, and cancer. Parallel to the action of COX-1/2 for the biosynthesis of prostaglandins from AA, lipoxygenases mediate the biosynthesis of leukotrienes and eoxins from AA, all of which are eicosanoids that play a significant role in inflammation and immune function . Of note, the ability for LOX-15 to generate eoxin has been identified as a novel pathway of inflammatory responses in mast cells and eosinophils  and as a promising novel target against asthma . Genetic ablation of LOX-12/15, but not LOX-5, was shown to protect against denervation-induced muscle atrophy . In the central nervous system, LOX-12/15 was shown to have increased expression in oligodendrocytes and microglia of periventricular leukomalacia , and disease phenotype was ameliorated by absence of LOX-12/15 in animal models of Alzheimer’s disease . The LOX-5 pathway has also been associated with Alzheimer’s disease and other neurodegenerative conditions . Although the mechanism of how LOX causes microglial activation and neuroinflammation remains to be elucidated, our results provided evidence suggesting that LOX activation in microglial cells plays a crucial role leading to induction of ROS and NO. To our knowledge, this is the first finding to biochemically connect cPLA2 pathway to oxidation and inflammatory responses in microglial cells through LOX. Future studies should further examine the specific involvement of LOX isoforms in proinflammatory gene expression and regulation of ROS production in microglial cells.
cPLA2 as a therapeutic target against neurological diseases
Since the 1990s, cPLA2 has been demonstrated to be a favorable target for intervention against a wide range of neurological diseases. Using an experimental stroke model, Bonventre et al. was the first to show that cPLA2 knockout mice suffered less ischemic damage and had smaller infarct volume after transient middle cerebral artery occlusion . Sanchez-Mejia et al. also demonstrated transgenic hAPP mice with cPLA2 knockout to exhibit significantly less cognitive deficit compared with cPLA2 intact transgenic hAPP mice, indicating a potential role of cPLA2 in the pathogenesis of Alzheimer’s disease . AACOCF3, a non-selective cPLA2 and iPLA2 inhibitor, was discovered to be an effective pharmacological inhibitor of PLA2. Due to its physicochemical properties, it can readily penetrate into cell membranes. In thrombin-stimulated platelets, in Ca2+ ionophore-stimulated human monocytic cells, and in interleukin 1-stimulated mesangial cells, all liberation of AA is essentially blocked at a concentration of 5 to 20 μM [74, 75]. Since the discovery and popularization of AACOCF3, more recent studies further demonstrated the administration of cPLA2 pharmacologic inhibitor to offer protective effect against multiple neurological diseases. This includes the amelioration of focal ischemic damage in experimental stroke , prevention of secondary tissue damage in experimental autoimmune encephalitis, an in vivo model for multiple sclerosis , as well as preservation of neuronal survival and retention of motor function in a mouse model of spinal cord injury [29, 76].
While most of the studies suggested and focused on the action of cPLA2 in the neurons in the event of neurodegeneration and neuronal apoptosis, less attention was given to the potential role of cPLA2 in the microglia cells. While microglia activation plays an important role to limit neuronal damage and phagocytose cellular debris and foreign pathogens, M1 activation of microglia cells can also promote microglia-induced neuronal damage and further propagate ongoing neuroinflammation. The results of this study had shed light on one potential mechanism of M1 microglia activation, which can potentially be targeted and controlled. Interestingly, inhibition of cPLA2 by AACOCF3 was able to abrogate the morphological changes elicited by LPS and IFNγ in WT primary microglial cells. We believe that cPLA2 inhibition not only prevents microglia activation but more importantly becomes a viable therapeutic strategy to impede neuronal cell death by limiting secondary neuronal damage. In this regard, inhibiting PLA2 cascade has been considered an essential strategy for opposing microglia activation  and discovering new and synthetic inhibitors for PLA2 will be an important future endeavor for understanding and treatment of neurological disorders .
This study demonstrated a crucial role of cPLA2 in the activation of microglial cells, specifically in LPS- and IFNγ-stimulated ROS and iNOS/NO production. In addition, cPLA2 also controls the morphological transformations associated with microglial activation. Upon looking at the downstream pathways, results show that LPS- and IFNγ-induced activation of ROS/NO is dependent on LOX-12/15 and not COX-1/2, thus offering new insights into the signaling pathway during microglia activation. Further studies are needed to better understand the molecular mechanisms underlying cPLA2 in microglial activation and how this may offer novel therapeutic options for the prevention and/or treatment of neuroinflammatory/neurodegenerative diseases.
We would like to express our appreciation for (1) Dr. Joseph V. Bonventre for providing the cPLA2 transgenic animals; (2) Yijia Zong for helping establish the protocol to isolate primary microglia from transgenic mice brains; (3) the Mouse Genetics Core in Washington University School of Medicine for assisting with the husbandry and genotyping for the iPLA2 transgenic animals used in this study; and (4) the Cellular Immunology Core in the University of Missouri for aiding in the flow cytometry protocol.
This publication was made possible by NIH Grants 2P01 AG08357 from NIA and P50AT006273 from the National Center for Complementary and Alternative Medicines (NCCAM), the Office of Dietary Supplements (ODS), and the National Cancer Institute (NCI), and NS074350 from the National Institute of Neurological Disorders and Stroke (NINDS). Its contents are solely the responsibility of the authors and do not necessarily represent the official views of the NIA, NCCAM, ODS, NCI, NINDS, or the National Institutes of Health.
Open AccessThis article is distributed under the terms of the Creative Commons Attribution 4.0 International License (http://creativecommons.org/licenses/by/4.0/), which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated.
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