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Journal of Neuroinflammation logoLink to Journal of Neuroinflammation
. 2008 May 19;5:17. doi: 10.1186/1742-2094-5-17

Neuroinflammatory response to lipopolysaccharide is exacerbated in mice genetically deficient in cyclooxygenase-2

Saba Aid 1, Robert Langenbach 2, Francesca Bosetti 1,✉
PMCID: PMC2409311  PMID: 18489773

Abstract

Background

Cyclooxygenases (COX) -1 and -2 are key mediators of the inflammatory response in the central nervous system. Since COX-2 is inducible by inflammatory stimuli, it has been traditionally considered as the most appropriate target for anti-inflammatory drugs. However, the specific roles of COX-1 and COX-2 in modulating a neuroinflammatory response are unclear. Recently, we demonstrated that COX-1 deficient mice show decreased neuroinflammatory response and neuronal damage in response to lipopolysaccharide (LPS).

Methods

In this study, we investigated the role of COX-2 in the neuroinflammatory response to intracerebroventricular-injected LPS (5 μg), a model of direct activation of innate immunity, using COX-2 deficient (COX-2-/-) and wild type (COX-2+/+) mice, as well as COX-2+/+ mice pretreated for 6 weeks with celecoxib, a COX-2 selective inhibitor.

Results

Twenty-four hours after LPS injection, COX-2-/- mice showed increased neuronal damage, glial cell activation, mRNA and protein expression of markers of inflammation and oxidative stress, such as cytokines, chemokines, iNOS and NADPH oxidase. Brain protein levels of IL-1β, NADPH oxidase subunit p67phox, and phosphorylated-signal transducer and activator of transcription 3 (STAT3) were higher in COX-2-/- and in celecoxib-treated mice, compared to COX-2+/+ mice. The increased neuroinflammatory response in COX-2-/- mice was likely mediated by the upregulation of STAT3 and suppressor of cytokine signaling 3 (SOCS3).

Conclusion

These results show that inhibiting COX-2 activity can exacerbate the inflammatory response to LPS, possibly by increasing glial cells activation and upregulating the STAT3 and SOCS3 pathways in the brain.

Introduction

Prostaglandin endoperoxide synthases or cyclooxygenases (COX-1 and COX-2) play a central role in the inflammatory cascade by converting arachidonic acid (AA), released from membrane phospholipids by a phospholipase A2 (PLA2), into prostaglandin endoperoxide H2, which in turn is converted to bioactive prostanoids by specific terminal synthases. The two COX isoforms share 60% homology in their amino acids sequence and have comparable kinetics; however they also show individual differences. COX-1 is normally constitutively expressed in most tissues and thought to be involved in homeostasis, whereas COX-2 is inducible upon inflammatory and other stimuli [1]. However, in the central nervous system (CNS), COX-1 and COX-2 are both constitutively expressed and COX-2 is mainly detected in the perinuclear, dendritic and axonal domains of neurons, particularly in cortex, hippocampus, amygdala and dorsal horn of the spinal cord of both rodent and human CNS [2-4]. In the CNS, COX-2 has been implicated in important physiological functions such as synaptic transmission, neurotransmitter release, blood flow regulation, and sleep/wake cycle [5-9].

Both COX-1 and COX-2 have been shown to play important roles in an inflammatory response, their contribution being different depending on the type of insult, the time after insult, and the tissue examined [6,10]. Because COX-2 is highly inducible by inflammatory stimuli it has been traditionally considered as the most appropriate target for anti-inflammatory drugs [2,11]. However, the exact role of each COX isoform in neuroinflammation is unclear. While we have recently reported that genetic deletion or pharmacological inhibition of COX-1 significantly ameliorate the neuroinflammatory response and brain injury following lipopolysaccharide (LPS) treatment [12], the role of COX-2 in the neuroinflammatory process remains controversial. For instance, COX-2 deficient (COX-2-/-) mice have been reported to be resistant to the febrile response induced by peripheral injection of LPS [13]. On the other hand, selective pharmacological inhibition of COX-2, but not of COX-1, increases the expression of several pro-inflammatory genes in the vascular associated cells and the parenchymal microglia after systemic injection of LPS [14].

In this study we examined the neuroinflammatory response of COX-2-/- and wild type (COX-2+/+) mice to intracerebroventricular (icv) injection of LPS, which is a model of direct activation of brain innate immunity [15-19].

LPS, a component of the outer cell wall of gram-negative bacteria, mediates its effect through the CD14 receptor, a glycosylphosphatidylinositol-linked membrane protein that is present on microglial cells. The LPS-CD14 complex, together with other adaptor proteins, binds to the toll-like receptor 4 (TLR4), which is present on microglia, but not on astrocytes, oligodendrocytes or cortical neurons [20]. This initiates a bifurcated signal transduction cascade that leads to the transcription of inflammatory and immune response genes, primarily via nuclear factor- κB (NF-κB) activation but also through c-Fos/c-Jun and Janus kinase (JAK)/signal transducer and activator of transcription 3 (STAT3)-dependent pathways [21]. The signaling events ultimately lead to the production of free radicals generated by NADPH oxidase, myeloperoxidase and inducible nitric oxide synthase (iNOS) in combination with cytokines and chemokines [22,23], which are mediators of the LPS-induced injury [15,16,24]. In this regard, previous data suggest that interleukin-1β (IL-1β) and tumor necrosis factor-α (TNF-α) can contribute to neuronal death in models of acute CNS injury as well as in chronic neurodegenerative disease [25].

In this study, we demonstrate that COX-2-/- mice are more susceptible than COX-2+/+ mice to LPS-induced neuronal injury and exhibit an increase in microglia and astrocyte activation, and increases in the expression of genes and proteins for inflammatory cytokines, chemokines, reactive oxygen species-generating enzymes, such as iNOS and NADPH oxidase, and in the expression of STAT3 and suppressor of cytokine signaling 3 (SOCS3) signaling molecules. COX-2+/+ mice chronically treated with celecoxib, a COX-2 selective inhibitor, also exhibit an increased neuroinflammatory response compared to untreated wild-type mice.

Materials and methods

Animals housing

Three-month-old male COX-2+/+ and COX-2-/- mice on a C57BL/6-129/Ola genetic background were used [26]. Mice were received at our animal facility at 6 weeks of age from a NIEHS colony maintained by Taconic Farms (Germantown, NY) with heterozygous by heterozygous breedings for greater than 35 generations. In order to prevent the inclusion of strain or genetic background confounders between COX deficient and wild type mice, all of the mice used in this study were progeny derived from heterozygous by heterozygous mating and therefore all contained the same strain and genetic background [26,27]. Mice were housed at 25°C in our animal facility with a 12 h light/dark cycle with free access to food and water. For celecoxib pretreatment, COX-2+/+ mice were given free access for six weeks to a diet containing 0 or 6000 ppm celecoxib, a COX-2 specific inhibitor, as previously described [28]. Briefly, celecoxib (Celebrex™) capsules (400 mg; Pfizer Inc, New York, NY) were obtained from the NIH Division of Veterinary Medicine and were incorporated into feed by Research Diets, Inc. (New Brunswick, NJ). All procedures were performed under a NICHD approved animal protocol in accordance with NIH guidelines on the care and use of laboratory animals.

LPS administration

Mice were anesthetized with ketamine (100 mg/kg) and xylazine (10 mg/kg, i.p.) and positioned in a stereotaxic apparatus (Kopf Instruments, Tujunga, CA). Vehicle (sterile phosphate buffer, 5 μl) or LPS (E. coli serotype 055:B5 (Sigma); 5 μg in 5 μl of sterile saline) was administered into the cerebral lateral ventricle using a 10 μl syringe with a 33 gauge needle (World Precision Instruments, Sarasota, FL) and a syringe pump (Stoelting, Wood Dale, IL) at a rate of 1 μl/min. This dose of LPS has been shown by us and by others to produce significant neuroinflammation when measured at 24 h [12,24,29]. The coordinates for the sterotaxic injections were -2.3 mm dorsal/ventral, -1.0 mm lateral, and -0.5 mm anterior/posterior from the bregma [30]. The needle was kept in this position for an additional 5 min after injection and then retrieved slowly from the brain.

Tissue preparation and histology

Twenty-four hours after LPS injection, mice were anesthetized with sodium pentobarbital (100 mg/kg, i.p.) and then rapidly perfused transcardially with 0.9% saline solution containing 0.5% sodium nitrate and heparin (10 U/ml), followed by ice cold 4% paraformaldehyde in 0.1 M phosphate buffer. After transcardiac perfusions, brains were rapidly removed, postfixed for 4 h, and then cryoprotected in 30% sucrose at 4°C. Frozen brains were cut into 30 μm coronal sections using a cryostat and stored at -20°C.

Neurodegeneration was assessed using Fluoro-Jade B (FJB), as previously described [31]. Briefly, mounted brain sections were dried for 4 h, rehydrated through graded concentrations of alcohol (100, 70%; 1 min each), and rinsed for 1 min in distilled water. Sections were dipped and shaken in potassium permanganate (0.06%) for 20 min, rinsed for 1 min in distilled water, dipped, and shaken in a solution containing 0.004% FJB (Histochem, Jefferson, AR), 0.1% acetic acid for 20 min. The slides were thereafter rinsed three times in distilled water (1 min each), dried, dipped in xylene, and coverslipped with Permount mounting medium (Fisher Scientific, Ottawa, Ontario) [31].

For immunohistochemistry, free-floating sections were rinsed three times in phosphate-buffered saline (PBS) (10 min each) and then pretreated with PBS containing 3% hydrogen peroxide for 10 min to block endogenous peroxidase activity. After PBS wash, brain sections were incubated once in PBS with 0.3% Triton X-100 and once in PBS containing 0.5% BSA for 30 min with gentle shaking. The sections were incubated overnight at 4°C with anti-mouse scavenger receptor A (SRA) (1:100; Serotec, Raleigh, NC) in PBS containing 5% normal serum; followed by treatment with a biotinylated secondary antibody (Vector Laboratories, Burlingame, CA) for 1 h in PBS plus 5% normal serum at room temperature, and then with the Vector ABC kit (Vector Laboratories) for 1 h at room temperature. The sections were visualized with the 3,3-diaminobenzidine tetrachloride (DAB; Vector Laboratories, Burlingame, CA). Mounted brain sections were dried for 4 h, dehydrated through graded concentration of alcohol, cleared in xylene, and coverslipped with Permount mounting medium (Fisher Scientific).

RNA extraction and quantitative real-time PCR

Brain total RNA was extracted using RNeasy Lipid Tissue Midi Kit (Qiagen, Valencia, CA, USA) as directed by the manufacturer. Total RNA extraction and reverse transcription were performed as previously described, using the Applied Biosystems Assay-On-Demand Gene Expression protocol with an ABI PRISM 7000 Sequence Detection System (Applied Biosystems, Foster City, CA) [32-34]. Briefly, five micrograms of total RNA were reverse transcribed using a High Capacity cDNA Archive kit (Applied Biosystems). Quantitative PCR for glial fibrillary acidic protein (GFAP), SRA1, TNF-α, IL-1β, interleukin 6 (IL-6), CCL2/monocyte chemoattractant protein-1 (MCP-1), CCL3/macrophage inflammatory protein 1 alpha (MIP-1α), iNOS, the NADPH oxidase subunits gp91phox and p67phox, mPGES-1, cPLA2, COX-1, NF-κB-P65, STAT3, and SOCS3, was performed using specific Taqman® probes (Applied Biosystems). Data were analyzed using the comparative threshold cycle (ΔΔ Ct) method [35]. Results were normalized with phosphoglycerate kinase 1 (Pgk1) as the endogenous control, and expressed as fold difference from the vehicle injected COX-2+/+ mice.

Western blotting

Western blot analyses were carried out as described previously [33] and nuclear proteins were prepared by using a compartmental protein extraction kit (Chemicon, Temecula) according to the manufacturer's protocol. Briefly, protein fractions were separated on Criterion gels (Bio-Rad), blotted onto a polyvinylidene difluoride membrane (Bio-Rad), and then immunoblotted with antibodies that recognize p67phox (1:500; BD Biosciences), phosphorylated STAT3 (p-STAT3 (Tyr 705), 1:500, Cell signaling, USA), STAT3 (1:1000 Cell signaling, USA), COX-1 (1:500 Cayman Chemicals, USA), and glyceraldehyde dehydrogenase (GAPDH, 1: 2000, Santa Cruz, CA, USA) to control for protein loading. Blotted proteins were detected and quantified using an Odyssey Infrared Imaging System (Li-Cor Biosciences, Lincoln, NB, U.S.A.). For IL-1β measurement, a 500 μl aliquot of the crude brain homogenate was centrifuged at 10,000 × g for 20 min at 4°C, and the supernatant was immediately assayed using an ELISA-based kit (mouse IL-1β/IL-1F2 Quantikine ELISA kit, R&D Biosystems, Minneapolis, USA). TNF-α and MIP-1α were measured in the brain supernatant (Searchlight® Sample testing service, Pierce Biotechnology, Woburn, MA, USA). Results were expressed as ng/g protein.

Statistics

Data were expressed as mean ± SEM and were analyzed with a two-way ANOVA. For Real-Time PCR results, the two-way ANOVA was performed on the log-transformed ΔΔCt. p values < 0.05 were considered statistically significant.

Results

Only COX-2-/- mice show FluorojadeB positive neurons 24 h after LPS

To address the hypothesis that LPS exerts different neurotoxic effects in the COX-2+/+ and COX-2-/- mice, we assessed neuronal damage in the brain 24 h after LPS injection using the fluorescent marker FJB, which selectively stains injured neurons [31]. LPS-injected COX-2-/- mice (Fig. 1) showed FJB-positive cells in the hippocampal area. In contrast, FJB-positive neurons were not detected in the hippocampus of vehicle-injected mice of each genotype and in LPS injected COX-2+/+ mice.

Figure 1.

Figure 1

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Effects of COX-2 deficiency on LPS-induced neuronal degeneration. Representative photomicrographs of FluoroJade-B staining in the hippocampus of COX-2+/+ and COX-2-/- mice 24 h after icv injection of LPS or vehicle. High magnification (10×) images of FluoroJade-B staining in the hippocampus are shown. The inset shows details of the neurons stained by FluoroJade-B in the hippocampus of COX-2-/- mice 24 h after icv injection of LPS (40× magnification). Bars represent 100 μm.

LPS-induced glial cell activation is increased in COX-2-/- mice

To determine glial cell response, we examined the expression of GFAP, a specific marker for astrocytes, and SRA, a specific marker for phagocytic microglia [36], 24 h after LPS injection, using quantitative real time PCR and immunohistochemistry. LPS markedly increased the expression of GFAP (Fig. 2A) and SRA mRNA (Fig. 2B) compared to vehicle injected mice, and the induction was higher in COX-2-/- than in COX-2+/+ mice.

Figure 2.

Figure 2

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Effects of COX-2 deficiency on LPS-induced expression of glial markers. Quantitative real time-PCR analysis of astrocyte marker GFAP (A) and microglia marker SRA mRNA (B) in COX-2+/+and COX-2-/- mice 24 h after icv injection of LPS or vehicle. Data are presented as mean ± SEM (n = 4-6). ***P < 0.001 compared to the corresponding vehicle-injected mice; #P < 0.05 compared to the LPS-injected COX-2+/+ mice. (C) Effects of COX-2 deficiency on LPS-induced activation of microglia. Representative photomicrographs of SRA immunohistochemistry in the striatum/caudate putamen and hippocampal area for COX-2+/+ and COX-2-/- mice 24 h after icv injection of LPS or vehicle. Bars represent 100 μm.

Then we determined the immunoreactivity to SRA. In vehicle-treated COX-2+/+ and COX-2-/- mice, no SRA immunoreactivity was seen (Fig. 2C). Intense immunoreactive SRA-positive microglia with enhanced staining intensity, enlarged cell bodies, and thickening of processes were observed 24 h after LPS injection in the cortical/caudate putamen and hippocampal area of COX-2+/+mice. In LPS-injected COX-2-/- mice, SRA-positive cells were numerous with higher cells retaining an enlarged cell body with thickening of ramified processes (Fig. 2C).

Expression of cytokines and chemokines is increased in COX-2-/- mice after LPS

The expression of cytokine and chemokine genes, such as TNF-α, IL-6, IL-1β, MIP-1α/CCL3, MCP-1/CCL2, was determined quantitatively using real time PCR. LPS significantly increased the expression of TNF-α (Fig. 3A), IL-6 (Fig. 3B), IL-1β (Fig. 3C), MIP-1α and MCP-1 (Fig. 3E) mRNA in both COX-2+/+ and COX-2-/- mice. However, the mRNA levels of these cytokines were higher in the COX-2-/-compared to COX-2+/+ mice (Fig. 3A–C and 3E). IL-1β was almost not detectable in the brain of vehicle-injected mice (Fig. 3D). Brain protein levels of IL-1β were also increased after LPS in both COX-2+/+ and COX-2-/- mice, and the increase was higher in the COX-2-/- mice (Fig. 3D). Brain protein levels of TNF-α and of MIP-1α were also significantly increased after LPS injection in COX-2-/-compared to COX-2+/+ mice (TNF-α: 3.9 ± 0.2, LPS injected COX-2-/- (n = 5) vs. 2.2 ± 0.6 ng/g protein, LPS injected COX-2+/+ (n = 3); MIP-1α: 340 ± 70, LPS injected COX-2-/-(n = 5) vs. 70 ± 41 ng/g protein, LPS injected COX-2+/+ (n = 3), p < 0.05).

Figure 3.

Figure 3

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Effects of COX-2 deficiency on LPS-induced expression of cytokines and chemokines. Quantitative real time-PCR analysis of TNF-α (A), IL-6 (B), IL-1β (C), and CCL3/MIP-1α and CCL2/MCP-1 (E) for COX-2+/+ and COX-2-/- mice 24 h after icv injection of LPS or vehicle. (D) ELISA-based quantification of IL-1β protein levels in the brain of COX-2+/+ and COX-2-/-mice 24 h after icv injection of LPS or vehicle. Data are presented as mean ± SEM (n = 4-6). ***P < 0.001 compared to the corresponding vehicle-injected mice; #P < 0.05, ##P < 0.01, ###P < 0.001 compared to the LPS-injected COX-2+/+ mice.

mRNA expression of mPGES-1 is increased in COX-2-/- mice after LPS

Brain mRNA levels of mPGES-1 were significantly increased by LPS, but the induction was significantly higher in the COX-2-/- mice compared to COX-2+/+ mice (Fig. 4A). In contrast, cPLA2 mRNA expression was increased by LPS to a similar extent in both COX-2+/+ and in COX-2-/- mice (Fig. 4B). COX-1 protein (Fig. 4C and 4D) and mRNA levels were not significantly changed by either LPS treatment or mouse genotype (COX-2+/+ mice: 0.8 ± 0.03 LPS vs. 1.0 ± 0.07 vehicle; COX-2-/- mice: 1.5 ± 0.41 LPS vs. 0.9 ± 0.07 vehicle; p > 0.05), suggesting that the enhanced neuroinflammatory response in COX-2-/- mice is not mediated by a compensatory induction in COX-1 after LPS. The expression of cPGES and mPGES-2 mRNA was not significantly different between COX-2+/+ and COX-2-/- mice after LPS injection (data not shown), suggesting that these enzymes are not involved in the enhanced neuroinflammatory response of COX-2-/- mice at the time point examined.

Figure 4.

Figure 4

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Effects of COX-2 deficiency on LPS-induced expression of enzymes involved in the arachidonic acid cascade. Quantitative real time-PCR analysis of mPGES-1 (A) and cPLA2 (B) for COX-2+/+ and COX-2-/- mice 24 h after icv injection of LPS or vehicle. (C) Quantification of COX-1 protein levels, relative to GAPDH internal loading control in the whole brain. (D) Representative immunoblot of COX-1 expression in COX-2+/+ and COX-2-/- mice 24 h after icv injection of LPS or vehicle. Data are presented as mean ± SEM (n = 4-6). ***P < 0.001 compared to the corresponding vehicle-injected mice; #P < 0.05 compared to the LPS-injected COX-2+/+ mice.

Expression of reactive oxygen species generating enzymes is increased in COX-2-/- mice after LPS

iNOS and NADPH oxidase are major sources of reactive oxygen species during the inflammatory process, and both are expressed in glial cells. We examined gene and protein expression of ROS-generating enzymes in COX-2-/- mice 24 h after LPS injection using quantitative real time-PCR and Western blotting. In response to LPS, COX-2-/- mice showed a higher increase in iNOS mRNA levels compared to COX-2+/+ mice (Fig. 5A). Similarly, mRNA levels of NADPH oxidase cytosolic subunit p67phox and membrane subunit gp91phox were significantly elevated at 24 h after LPS injection in both genotypes compared with vehicle-injected controls (Fig. 5B and 5C). COX-2-/- mice showed a higher increase in the expression of p67phox and gp91phox mRNA than COX-2+/+ mice (Fig. 5B and 5C). Western blotting analysis confirmed that protein level of the p67phox subunit was higher in the COX-2-/- mice compared to the COX-2+/+ mice after LPS (Fig. 5D and 5E).

Figure 5.

Figure 5

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Effects of COX-2 deficiency on LPS-induced expression of ROS-generating enzymes. Quantitative real time-PCR analysis of iNOS (A), gp91phox (B) and p67phox mRNA (C) for COX-2+/+ and COX-2-/- mice that received icv injection of LPS or vehicle 24 h before sacrifice. (D) Quantification of p67phox protein levels, relative to GAPDH internal loading control in the whole brain. (E) Representative immunoblot of p67phox expression in COX-2+/+ and COX-2-/- mice 24 h after icv injection of LPS or vehicle. Data are presented as mean ± SEM (n = 4-6). ***P < 0.001 compared to the corresponding vehicle-injected mice; #P < 0.05, ##P < 0.01 compared to the LPS-injected COX-2+/+ mice.

Phosphorylated STAT3 and the mRNA expression of STAT3 and SOCS3, but not of NF-κB, are increased in COX-2-/- mice after LPS

Activation of the transcription factors NF-κB and STAT3 plays a critical role in the production of inflammatory mediators by activated microglia [12]. STAT signaling is tightly regulated by its negative regulators, suppressors of cytokine signaling (SOCS), and is controlled by STAT phosphorylation [37]. To determine the transcriptional mechanism underlying the increased inflammatory response to LPS observed in the COX-2-/- mice, we examined NF-κB p65 and STAT3 levels. The mRNA expression of NF-κB (Fig. 6A) was increased similarly in COX-2+/+ and COX-2-/- mice after LPS. The expression of STAT3 and SOCS3 mRNA was also significantly increased 24 h after LPS injection in both genotypes compared to the vehicle-injected COX-2+/+ mice (Fig. 6B and 6C), but the increase was significantly higher in COX-2-/- mice than in COX-2+/+ mice. Phosphorylated STAT3 was not detected in the brain nuclear fraction of vehicle-injected mice (Fig. 6D and 6E); however, after LPS, phosphorylated STAT3 protein level increased in both genotypes, but was increased to a greater extent in COX-2-/- mice (Fig. 6D and 6E).

Figure 6.

Figure 6

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Effects of COX-2 deficiency on LPS-induced expression of transcription factors NF-κB and STAT3, and SOCS3. Quantitative real time-PCR analysis of NF-κB (A), SOCS3 (B) and STAT3 mRNA (C) for COX-2+/+ and COX-2-/- mice 24 h after icv injection of LPS or vehicle. (D) Quantification of phosphorylated STAT3 (Tyr 705) protein levels, relative to the total STAT3 in the brain nuclear fraction. (E) Representative immunoblot of P-STAT3 expression in COX-2+/+ and COX-2-/- mice 24 h after icv injection of LPS or vehicle. Data are presented as mean ± SEM (n = 4-6). *P < 0.05, **P < 0.01, ***P < 0.001 compared to the corresponding vehicle-injected mice; ##P < 0.01 compared to the LPS-injected COX-2+/+ mice.

Pretreatment of COX-2+/+ mice with celecoxib for 6 weeks increases LPS-induced brain IL-1β level, NADPH oxidase subunit p67phox, and phosphorylated STAT3

Brain COX-1 protein levels were not significantly changed by LPS treatment either in COX-2+/+ or in celecoxib-treated mice (Fig. 7A, COX-2+/+ mice: 0.041 ± 0.009 LPS vs. 0.033 ± 0.003 vehicle; celecoxib-treated COX-2+/+ mice: 0.043 ± 0.0.008 LPS vs. 0.038 ± 0.004 vehicle; p > 0.05). COX-2+/+ mice pretreated with celecoxib showed a significant increase in brain IL-1β protein level after LPS, compared to untreated mice (Fig. 7B). The protein levels of p67phox (Fig. 7C and 7D) and phosphorylated STAT3 after LPS (Fig. 7E and 7F) were also higher in the celecoxib-treated mice compared to untreated mice.

Figure 7.

Figure 7

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Effects of chronic pretreatment with celecoxib (6000 ppm for 6 weeks) on LPS-induced brain IL-1β levels, the expression of COX-1, p67phox NADPH oxidase subunit and the phosphorylated STAT3. (A) Representative immunoblot of COX-1 protein levels, relative to GAPDH internal loading control, in the whole brain of COX-2+/+ and celecoxib-treated COX-2+/+ mice 24 h after icv injection of LPS or vehicle. (B) ELISA based immunoassay for brain IL-1β in celecoxib-treated mice (n = 7) and untreated COX-2+/+ mice (n = 4). (C) Quantification of p67phox protein levels, relative to GAPDH internal loading control in the whole brain with representative immunoblot (D) in celecoxib-treated mice and untreated COX-2+/+ mice (n = 4). (E) Quantification of phosphorylated STAT3 (Tyr 705) protein levels, relative to the total STAT3 in the brain nuclear fraction and the representative immunoblot (F) in celecoxib-treated mice and untreated COX-2+/+ mice (n = 4). All data are expressed as mean ± SEM. *P <0.05, **P < 0.01, ***P < 0.001 compared to the corresponding vehicle-injected mice; #P < 0.05, ###P < 0.001 compared to the LPS-injected COX-2+/+ mice.

Discussion

In this study we demonstrate for the first time that genetic deletion of COX-2 enhanced the neuroinflammatory response and increased the susceptibility to neuronal damage induced by centrally injected LPS. We also showed that chronic treatment with a selective COX-2 inhibitor, celecoxib, also increases LPS-induced protein levels of IL-1β, a major proinflammatory cytokine, of phosphorylated STAT3, a transcription factor involved in the progression of the inflammatory cascade, and of NADPH oxidase subunit p67phox, a marker of oxidative stress. We have previously demonstrated that this chronic dosing paradigm of celecoxib (6000 ppm for 6 weeks) leads to a plasma concentration of 18.2 ± 5.8 μg/ml [28]. Assuming 98% binding of celecoxib to plasma proteins and that only free celecoxib can cross the blood brain barrier [38], brain concentration of celecoxib is approximately 640 nM, well above the IC50 (39 nM) of celecoxib for COX-2 [28]. These plasma concentrations are within the same order of magnitude of steady state concentrations (2–3 μg/ml) observed in humans after acute administration of 400–800 mg of celecoxib, doses clinically used for the treatment of rheumatoid arthritis and familial adenomatous polyposis [39].

In this study, FJB-positive neurons were only observed in the COX-2-/- mice, suggesting that COX-2 deletion increases the susceptibility to LPS-induced neurodegeneration. There is a conflicting view about the role of COX-2 in neurodegeneration and neurotoxicity [40]. For instance, COX-2 inhibition is believed to be neuroprotective in models such as MPTP (1-methyl 4-phenyl 1,2,3,6-tetrahydropyridine), quisquallic acid induced damage [41,42], and centrally injected NMDA-induced neurotoxicity [43,44]. However, in these studies, where the toxins directly damage neurons, COX-2-mediated cytotoxicity does not appear to be linked to the inflammatory response [41]. On the other hand, pre-treatment with COX-2 inhibitors or genetic deletion of COX-2 has been shown to increase seizure activity and neuronal damage in response to kainate [28,45], and to exacerbate endotoxin-induced ocular inflammation [46] and tissue damage in ConA- and acetaminophen-induced hepatotoxicity [47,48]. Another study reported, in support of our observations, that selective pharmacological inhibition of COX-2 with NS-398 increases the transcription of inflammatory genes (mPGES-1, TLR2, CD14, MCP-1) in vascular associated brain cells and parenchymal microglia after systemic injection of LPS [14]. While these conflicting data highlight the importance of investigating the distinct roles of COX-1 and COX-2 in physiology and pathology, our findings suggest that COX-2-derived products selectively mediate a protective effect in the development and/or the resolution of inflammation in the brain after endotoxin activation of the innate immune system. In this regard, a recent review emphasizes that COX-2 mediates neuroprotection via specific anti-inflammatory lipid mediators [49]. Furthermore, Gilroy and colleagues demonstrated that selective COX-2 inhibitors, by blocking the production of PGE2 and PGD2, disturbed the resolution phase of inflammation, leading to delay in return to homeostasis [50].

COX-1 protein levels were not significantly changed by LPS in either COX-2-/- or celecoxib-treated mice compared to COX-2+/+ mice, indicating that the increased neuroinflammatory response was not due to an increased compensatory expression of COX-1 in response to LPS when COX-2 is either genetically abrogated or pharmacologically inhibited. Increases in microglial activation and in the induction of cytokines and chemokines in the COX-2-/- mice could contribute to the susceptibility to LPS-induced damage. Overexpression of chemokines, small pleiotropic chemoattractant cytokines that promote leukocytes activation and migration, has been recently implicated in many neurological disorders including multiple sclerosis, and Alzheimer's disease [51,52]. The overexpression of chemokines observed in the COX-2-/- mice after LPS may increase the leukocytes and monocytes recruitment in the inflamed brain and cause neuronal damages, in the absence of a "switch off" mechanism. The increased expression of cytokines could be due to the incapacity of the tissue to resolve the inflammation, leading to a persistent activation of the inflammatory cascade. One possibility is that COX-2 deletion or inhibition leads to a reduction in anti-inflammatory mediators or neurotrophic factors, which would impair the brain ability to resolve the inflammation.

iNOS and NADPH oxidase may also contribute to microglia-mediated LPS induced neurotoxicity by increasing the production of extracellular reactive oxygen and nitrogen species, which, in turn, stimulate the microglial release of pro-inflammatory mediators that, like radical oxygen species, are toxic to neurons [53,54]. In this regard, NADPH inhibitors suppress LPS-induced expression of iNOS, IL-6, IL-1β and TNF-α in glial cells in vitro [55] and NADPH oxidase has been shown to regulate COX-2 mediated PGE2 production in cultured microglia [56].

The JAK/STAT pathway is a key player in the intracellular response to cytokines. SOCS3 is a potent inhibitor of the JAK/STAT signaling cascade, negatively regulating signal transduction pathways mediated by a variety of cytokines. SOCS3 has been suggested to play a critical role in integrating the neuroimmunoendocrine circuits [57]. Although NF-κB p65 expression were similar in COX-2+/+ and COX-2-/- mice after LPS, we found that the mRNA expression of STAT3 and the levels of phosphorylated STAT-3 were significantly higher in the COX-2-/- mice compared to wild type mice. SOCS3 was also upregulated in the COX-2-/- mice compared to COX-2+/+ mice after LPS. SOCS3 is a negative modulator of inflammatory cytokine signaling [58] and can be induced by inflammatory stimuli such as LPS, TNF-α and IL-6 [58,59]. SOCS3 mRNA up-regulation in the COX-2 deficient mice can thus be viewed as the consequence of the higher cytokine production in these mice after LPS. In this regard, SOCS3 overexpression has been shown to lead to neuroblastoma cell death [60]. Overall, our data indicate a dysregulation of the cytokine signaling pathway in the COX-2-/- mice, which may mediate the increased neuroinflammatory response.

While independent epidemiological studies indicate that non steroidal anti-inflammatory drugs (NSAIDs) administration prevents or delays the onset and risk of developing Alzheimer's disease [61-63], clinical trials using COX-2 selective inhibitors in patients with mild to severe cognitive impairment, have been unsuccessful to date [64-67], with the exception of a small double blind, placebo-controlled study with indomethacin, a preferential COX-1 inhibitor [68]. We have recently demonstrated that genetic deletion or pharmacological inhibition of COX-1 significantly attenuates glial cells activation and the neuroinflammatory response, oxidative stress and neuronal damage in response to icv injected LPS [12]. Our results show that while COX-1 selective inhibition may be beneficial, selective inhibition of COX-2 appears not to be beneficial in neurodegenerative diseases with a marked inflammatory component and may explain the failure of selective COX-2 inhibitors to protect AD patients from cognitive decline in clinical trials [64-67].

Conclusion

These findings altogether indicate that the two COX isoforms display opposite roles in the brain during the acute neuroinflammatory process and that COX-2 inhibition worsens the inflammatory response to LPS, suggesting a neuroprotective function of COX-2-derived products. In this regard, further investigations are warranted to identify which specific COX-2 products may mediate the neuroprotective effects and more research should be focused on COX-1 selective inhibitors for the treatment of neurological and neurodegenerative diseases with an inflammatory component.

Abbreviations

AD: Alzheimer's disease; ANOVA: analysis of variance; BSA: bovine serum albumin; COX: cyclooxygenase; CNS: central nervous system; DAB: 3,3-diaminobenzidine tetrachloride; ELISA: enzyme linked immunosorbent assay; GAPDH: glyceraldehyde dehydrogenase; GFAP: glial fibrillary acidic protein; icv: intracerebroventricular; IL-1β: interleukin1 beta; IL-6: interleukin 6; iNOS: inducible nitric oxide synthase; JAK: Janus kinase; LPS: lipopolysaccharide; MCP-1: monocyte chemoattractant protein-1; MIP-1α: macrophage inflammatory protein 1 alpha; mPGES-1 or -2: microsomal prostaglandin E synthase-1 or -2; cPGES: cytosolic prostaglandin E synthase; NF-κB: nuclear factor- κB; PBS: phosphate-buffered saline; PGD2: prostaglandin D2; PGE2: prostaglandin E2; PLA2: phospholipase A2; ROS: reactive oxygen species; SOCS3: suppressors of cytokine signaling 3; SRA: scavenger receptor A; STAT3: signal transducer and activator of transcription 3; TNF-α: Tumor Necrosis Factor alpha.

Competing interests

The authors declare that they have no competing interests.

Authors' contributions

SA performed the experiments, contributed to study design and data analysis and wrote the manuscript. RL provided the COX-2+/+ and COX-2-/-mice and reviewed the manuscript. FB directed the work, contributed to study design, reviewed the data, and wrote the manuscript. All authors read and approved the final manuscript.

Acknowledgments

Acknowledgements

This work was supported by the Intramural Research Programs of the National Institute on Aging and the National Institute of Environmental Health Sciences, National Institutes of Health. We thank Drs. Sang-Ho Choi and Christopher D. Toscano for useful experimental suggestions and discussion and Dr. Alan B. Zonderman for statistical help.

Contributor Information

Saba Aid, Email: aidsab@mail.nih.gov.

Robert Langenbach, Email: langenb1@niehs.nih.gov.

Francesca Bosetti, Email: frances@mail.nih.gov.

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