Research ArticleImmunology

Purinergic Signaling: A Fundamental Mechanism in Neutrophil Activation

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Science Signaling  08 Jun 2010:
Vol. 3, Issue 125, pp. ra45
DOI: 10.1126/scisignal.2000549


Efficient activation of neutrophils is a key requirement for effective immune responses. We found that neutrophils released cellular adenosine triphosphate (ATP) in response to exogenous stimuli such as formylated bacterial peptides and inflammatory mediators that activated Fcγ, interleukin-8, C5a complement, and leukotriene B4 receptors. Stimulation of the formyl peptide receptor (FPR) led to ATP release through pannexin-1 (panx1) hemichannels, and FPRs colocalized with P2Y2 nucleotide receptors on the cell surface to form a purinergic signaling system that facilitated neutrophil activation. Disruption of this purinergic signaling system by inhibiting or silencing panx1 hemichannels or P2Y2 receptors blocked neutrophil activation and impaired innate host responses to bacterial infection. Thus, purinergic signaling is a fundamental mechanism required for neutrophil activation and immune defense.


Polymorphonuclear neutrophils (PMNs) form the first line of defense against invading pathogens; however, in addition to their beneficial actions in host defense, neutrophils are also involved in pathophysiological processes that lead to damage of host tissue in inflammatory diseases, sepsis, and ischemia-reperfusion injury after severe trauma and hemorrhage (1). Migration, degranulation, and the respiratory burst are key functional responses that enable PMNs to accomplish their tasks in host defense. These functional responses are triggered by receptors that recognize bacterial peptides, such as N-formyl-Met-Leu-Phe (fMLP), or innate inflammatory mediators, such as interleukin-8 (IL-8), leukotriene B4 (LTB4), and the complement product C5a, which orchestrate the responses of PMNs during inflammation and host defense (24). Similar to the formyl peptide receptors (FPRs), all of these PMN receptors belong to the G protein–coupled receptor (GPCR) superfamily. GPCRs use heterotrimeric guanine nucleotide–binding proteins (G proteins) to trigger downstream processes, including mobilization of calcium ions (Ca2+) and mitogen-activated protein kinase (MAPK) signaling, that induce functional cell responses. However, other receptors that are unrelated to GPCRs, such as the Fcγ receptors (FcγRs), also play critical roles in host defense by eliciting the phagocytosis and killing of invading bacteria.

Intracellular adenosine triphosphate (ATP) serves as a source of energy that drives virtually all cell functions; however, when released into the extracellular space, ATP serves as an intercellular messenger or an autocrine mediator that regulates cell functions. Through paracrine and autocrine mechanisms and the activation of purinergic receptors, ATP and its metabolites, including adenosine, modulate the biological functions of mammalian cells (59). Purinergic receptors are separated into two families: P1 adenosine receptors and P2 nucleotide receptors, which are further divided into the P2X and P2Y receptor subfamilies. The P2X receptor subfamily consists of seven members that function as ATP-gated ion channels, and the P2Y receptor subfamily comprises eight members that are GPCRs and recognize ATP, uridine triphosphate, and related molecules (911). We previously found that extracellular ATP controls chemotaxis of PMNs through P2Y2 receptors (12). Here, we show that ATP is released by pannexin-1 (panx1) hemichannels and that autocrine feedback through P2Y2 receptors is an essential purinergic signaling mechanism that is required for the activation of PMNs by a wide range of extracellular stimuli and regulates the responses of PMNs in immune defense and inflammation.


Stimulation of FPR triggers the release of ATP through maxi-anion channels and panx1 hemichannels

Stimulation of FPR causes the rapid release of ATP from PMNs (12). Mammalian cells can release cellular ATP through various mechanisms. Among these, release through connexin and pannexin hemichannels and maxi-anion channels has been observed in different cell types (1316). The human tweety homolog 1 (hTTYH1) and hTTYH3, which encode maxi-anion channels, are human homologs of a gene located in Drosophila flightless and are expressed in human leukocytes (15). Maxi-anion channels are associated with large-conductance chloride currents and can facilitate the release of ATP from mammalian cells (17). The various pannexin and connexin gap junction proteins form hemichannels that release ATP from leukocytes (14, 16). Cx43 hemichannels facilitate the release of ATP from PMNs, whereas panx1 hemichannels are involved in the release of ATP from T lymphocytes (14, 16). Through real-time reverse transcription polymerase chain reaction (RT-PCR) analysis, we found that human PMNs, undifferentiated neutrophil-like HL-60 cells, and differentiated HL-60 cells (dHL-60) expressed the genes encoding TTYH3 and panx1, but not those encoding TTYH1 or Cx43 (Fig. 1A). Consistent with these data, immunocytochemistry experiments revealed that human PMNs contained TTYH3 and panx1, but neither TTYH1 nor Cx43 (Fig. 1, B and C). We found that fMLP induced the translocation of panx1 to the leading edge in 80 ± 16% of polarized PMNs, which was identified by staining of the F-actin–rich leading edge of the cells with phalloidin (Fig. 1, C and D). Staining of cells with antibodies against panx1 and FPR revealed that panx1 colocalized extensively with FPR at the leading edge of polarized PMNs, where the greatest extent of F-actin staining was observed (Fig. 1D). By contrast, TTYH3 channels colocalized with FPR only in segregated foci that remained more uniformly distributed across the cell surface (fig. S1).

Fig. 1

ATP release channels in PMNs. (A) The abundance of mRNAs for the TTYH1 and TTYH3 maxi-anion channels, Cx43, and panx1 in human brain, primary human PMNs, and HL-60 cells, before and after differentiation (dHL-60) with 1.3% DMSO for 3 days, was estimated by real-time RT-PCR. nt, not tested; nd, not detected. Values are expressed as means ± SD, and data are representative of four experiments. (B) Immunostaining of primary human PMNs with antibodies against TTYH1, TTYH3, and Cx43. (C) Immunostaining of panx1 on primary human PMNs that were either unstimulated or stimulated with fMLP (1 nM). (D) Colocalization of F-actin (red), panx1 (green), and FPR (blue) in unpolarized human PMNs and in PMNs that were polarized by stimulation with fMLP (1 nM) that was added uniformly for 10 min. The images shown in (B) and (D) are representative of experiments performed at least twice with cells from different donors. The images in (C) are representative of at least three separate experiments.

panx1 and TTYH3 are sensitive to the anion channel inhibitor 4,4′-diisothiocyanatostilbene-2,2′-disulfonic acid (DIDS) (15, 18). We found that DIDS dose-dependently blocked fMLP-induced release of ATP and functional cell responses, including production of the adhesion molecule CD11b, migration of PMNs, and oxidative burst (Fig. 2, A and C). These results indicated that the stimulation of PMN responses by FPR required the release of cellular ATP through DIDS-sensitive panx1 or TTYH3 channels. The effectiveness with which DIDS inhibited the various cell functions varied, with half-maximal suppression of the production of CD11b, migration, and oxidative burst at DIDS concentrations of 5, 30, and 50 μM, respectively. This suggested that different functional responses differed with regard to their requirements for purinergic signaling and the involvement of ATP or adenosine, which is formed by ectonucleotidases that could also be affected by DIDS (fig. S2) (19, 20).

Fig. 2

Maxi-anion and panx1 channels mediate the FPR-induced release of ATP from PMNs. (A and B) The effects of DIDS, CBX, 10panx1, or a nonsense control peptide on the release of ATP from human PMNs in response to FPR stimulation with 100 nM fMLP for 3 min were examined. (C to E) The effects of DIDS, CBX, 10panx1, or nonsense control peptide on the functional responses of human PMNs stimulated with fMLP were determined. (F) Effect of knocking down TTYH3 on ATP release and oxidative burst of dHL-60 cells in response to fMLP. Values in all panels are expressed as means ± SD and data are representative of individual experiments with cells from at least three different donors. *P < 0.05.

To further evaluate the role of pannexin hemichannels, we used carbenoxolone (CBX), a more specific inhibitor of gap junction channels (18), and 10panx1, a mimetic blocking peptide that selectively inhibits panx1 hemichannels (16, 21). CBX dose-dependently suppressed fMLP-induced ATP release and functional PMN responses (Fig. 2, B and D). Ectonucleotidase activity can affect PMN responses by hydrolyzing extracellular ATP (22). In contrast to DIDS, CBX did not affect ectonucleotidase activity or the ability of PMNs to hydrolyze extracellular ATP (fig. S2). 10panx1 reduced FPR-induced ATP release and functional responses, whereas a control peptide (23) had little effect on these responses (Fig. 2, B and E). Whereas knockdown of TTYH3 with small interfering RNA (siRNA) reduced FPR-induced ATP release by 70% relative to that in control cells, the oxidative burst of HL-60 cells was only marginally affected (Fig. 2F). These results showed that TTYH3 and pannexin hemichannels both facilitated the release of ATP but that only panx1-mediated release of ATP seemed to play a role in FPR-induced functional responses. Treatment of PMNs with 10panx1, DIDS, or CBX reduced FPR-induced release of ATP by no more than 80%, which suggested that the remaining 20% was mediated by unrelated mechanisms. However, knockdown of TTYH3 channels in dHL-60 cells blocked the release of ATP by 70% relative to that of control cells, which indicated that there were either complex interactions between panx1- and TTYH3-induced ATP release or differences between PMNs and dHL-60 cells with regard to the contributions of these two channels to the release of ATP.

Extracellular ATP and P2Y2 receptors are required for FPR-induced activation of PMNs

Enzymes that hydrolyze extracellular ATP block the migration of PMNs (12). This observation and our data indicated that the release of ATP and autocrine feedback through ATP receptors were essential steps that linked the stimulation of FPRs with subsequent functional responses of PMNs. To study how released ATP influenced downstream signaling events triggered by FPR, we assessed intracellular Ca2+ mobilization in PMNs that were loaded with the intracellular Ca2+ probe Fura-2-AM. We found that inhibition of ATP release with CBX or 10panx1 or elimination of released ATP with apyrase dose-dependently inhibited FPR-induced Ca2+ mobilization in PMNs, whereas a control peptide (23) had little effect on Ca2+ responses (Fig. 3A). Furthermore, CBX and 10panx1 did not affect ATP-induced Ca2+ mobilization, indicating that these inhibitors blocked the FPR-induced release of ATP and did not directly affect P2 receptor–induced Ca2+ mobilization (fig. S3). Compared to CBX or 10panx1, relatively high concentrations of apyrase (5 to 20 U/ml) were needed to suppress the mobilization of Ca2+. This suggested that apyrase was less potent than CBX and 10panx1 in blocking purinergic signaling, because apyrase must compete with purinergic receptors for released ATP, whereas CBX and 10panx1 inhibit the upstream release of ATP and thus more effectively intercept purinergic signaling in response to the stimulation of FPRs. However, we observed that CBX and 10panx1 did not completely block Ca2+ mobilization, which suggested that Ca2+ mobilization depended on both purinergic signaling and direct FPR-induced pathways that were independent of purinergic receptors.

Fig. 3

FPR-induced Ca2+ mobilization and MAPK activation in human PMNs require the release of ATP. (A) Intracellular Ca2+ mobilization in response to fMLP (10 nM) in human PMNs pretreated with the indicated concentrations of apyrase, CBX, or 10panx1. Data are expressed as relative fluorescence units (RFU). (B) Effect of pretreatment of human PMNs with the indicated concentrations of CBX or apyrase on fMLP-stimulated activation of ERK, which was determined by assessing the ratio of the abundance of phosphorylated ERK (pERK) to that of total ERK protein. The data are representative of individual experiments with cells from four donors for (A) and three donors for (B).

Next, we tested whether the release of ATP was required for FPR-induced activation of extracellular signal–regulated kinase (ERK). CBX and apyrase dose-dependently reduced the activation of ERK (Fig. 3B). This indicated that ERK activation, like Ca2+ signaling, depended on the release of ATP. We used the P2 receptor antagonist suramin [8,8′-(carbonylbis(imino-4,1-phenylenecarbonylimino-4,1-phenylenecarbonylimino))bis-1,3,5-naphthalenetrisulfonic acid] to evaluate the role of purinergic receptors in FPR-induced cell signaling and functional PMN responses. Suramin dose-dependently reduced degranulation, oxidative burst, and chemotaxis, as well as the activation of ERK and the mobilization of Ca2+ (Fig. 4, A to C), indicating that P2 receptors were indispensable for the activation of PMNs. P2Y2 receptors are the most abundant P2 receptor subtype in human PMNs and dHL-60 cells (12). We found that knockdown of P2Y2 receptors, which reduced the abundance of P2Y2 messenger RNA (mRNA) by >80% in dHL-60 cells (fig. S4A), markedly inhibited FPR-induced Ca2+ mobilization and oxidative burst (Fig. 4, D and E). Thus, P2Y2 receptors were central to the activation of PMNs in response to stimulation of FPRs.

Fig. 4

P2 purinergic receptors are required for FPR-induced cellular responses in human PMNs. (A) The effects of the P2 receptor antagonist suramin on the functional responses of human PMNs to fMLP were examined. (B) The effect of suramin on Ca2+ signaling in PMNs in response to fMLP was examined. (C) The effect of suramin on fMLP-induced activation of ERK in PMNs was determined. (D and E) The effect of knockdown of P2Y2 receptors in dHL-60 cells on FPR-induced Ca2+ signaling and oxidative burst, which was assessed by flow cytometric analysis of Fluo-3 and DHR, respectively, was examined. Data are expressed as a percentage of controls treated with nonsense siRNA. Values are expressed as means ± SD [(A) and (E)] and the data are representative of at least three individual experiments with similar results. *P < 0.05.

FPR and P2Y2 receptors colocalize on the surface of PMNs

Rapid responses of the purinergic signaling systems described earlier require the close proximity of FPR, panx1, and P2Y2 receptors to effectively convey extracellular cues to functional responses. As shown earlier, panx1 colocalizes with FPR (Fig. 1D). We examined whether P2Y2 receptors also colocalized with FPR by cotransfecting dHL-60 cells with plasmids encoding P2Y2 tagged with enhanced cyan fluorescent protein (ECFP) and FPR tagged with enhanced yellow fluorescent protein (EYFP). FPR and P2Y2 indeed colocalized extensively on the surface of unstimulated dHL-60 cells (Fig. 5 and movies S1 and S2). After stimulation with fMLP to induce polarization, P2Y2 and FPR remained colocalized and were found across the surface of dHL-60 cells; however, colocalization was not observed in some subcellular structures, suggesting that FPR and P2Y2 associated with different cytosolic granules or organelles (Fig. 5 and fig. S5). Together, our findings show that FPR and P2Y2 form tight spatiotemporal associations that enable effective purinergic signaling and may serve to amplify FPR-induced activation signals through autocrine purinergic feedback loops.

Fig. 5

FPR and P2Y2 receptors colocalize on the cell surface. (A) dHL-60 cells were cotransfected with plasmids encoding P2Y2-ECFP and FPR-EYFP, and receptor distribution was assessed by confocal laser scanning microscopy. (B) The degree of receptor colocalization in different regions of interest (ROIs) was evaluated by regression analysis. ROI 1, ROI 2, and ROI 3 indicate areas with different degrees of receptor colocalization shown in the rightmost image in (A). The data are representative of more than three individual experiments.

Purinergic signaling is a fundamental activation process in PMNs

Our findings thus far indicated that signaling and functional responses to fMLP required the release of ATP and autocrine feedback through P2Y2. We tested whether similar purinergic feedback mechanisms controlled the responses of PMNs to other extracellular stimuli. FcγRs enable PMNs to recognize and phagocytose opsonized particles. We found that stimulation of FcγR also triggered the release of ATP. Similar to our findings with FPR, treatment with DIDS or CBX or inhibition of P2 receptors inhibited FcγR-induced release of ATP, formation of superoxide, and phagocytosis of opsonized bacteria (Fig. 6, A to C). Moreover, stimulation of PMNs through receptors for IL-8, C5a, and LTB4 also induced the release of ATP, and the activation of ERK in response to these stimuli was blocked by DIDS and CBX (Fig. 6, D to F). Thus, purinergic signaling did not seem to be restricted to FPR signaling but appeared to constitute a fundamental mechanism that was involved in the activation of PMNs by infectious and inflammatory extracellular stimuli that triggered a range of GPCRs and other cell surface receptors. The physiological importance of purinergic signaling for innate immune defense is underlined by our finding that PMNs from P2RY2 knockout (P2Y2 KO) mice showed impaired FPR-induced cell responses, for example, the expression of CD11b on the cell surface (Fig. 7A). In addition, we found that chemotaxis of PMNs was diminished in P2Y2 KO animals compared to that in wild-type mice (24) and that P2Y2 KO mice were less capable than their wild-type counterparts to contain bacterial infections, which resulted in substantially higher bacterial counts in the peritoneal cavities and in the livers, lungs, and spleens of infected P2Y2 KO mice relative to those in wild-type control mice (Fig. 7B).

Fig. 6

ATP release and autocrine feedback through purinergic receptors are a general requirement for the activation of PMNs. (A and B) Effects of DIDS, suramin, and CBX on ATP release and oxidative burst in human PMNs stimulated by ligation of FcγRs with IgG1 antibodies (5 μg/ml). (C) Effects of DIDS (100 μM), suramin (100 μM), and CBX (20 μM) on the phagocytosis of opsonized bacteria by human PMNs. (D) ATP release by human PMNs stimulated with fMLP (100 nM, 3 min), C5a (10 ng/ml, 2 min), LTB4 (10 nM, 1 min), IL-8 (10 ng/ml, 2 min), or IgG1 (5 μg/ml, 10 min). Values are expressed as the mean ± SD. (E and F) Effects of DIDS or CBX on the activation of ERK in human PMNs that were stimulated with IL-8 (10 ng/ml, 2 min) or LTB4 (10 nM, 1 min). The data are representative of individual experiments with cells from at least three different donors.

Fig. 7

P2Y2 receptors are required for immune defense in a mouse model of peritoneal infection. (A) Production of CD11b in PMNs from wild-type (WT) controls and P2Y2 KO mice. The abundance of CD11b on Gr-1–positive PMNs was determined 2 hours after induction of infection by CLP (n = 5 mice in each group). (B) Bacterial concentrations expressed as colony-forming units per milliliter (CFU/ml) in peripheral blood, peritoneal lavage fluid, and extracts from liver, lung, and spleen of WT or P2Y2 KO mice were determined 3 hours after CLP (n = 6 mice in each group). Data are expressed as means ± SD. *P < 0.05; **P < 0.001.


Whereas PMNs play an important role in protecting the host from infections, they are also responsible for tissue damage in the host that occurs in a number of inflammatory diseases, such as reperfusion injury, rheumatoid arthritis, inflammatory bowel disease, and asthma (1, 25). To devise effective therapeutic approaches that reduce PMN-induced tissue damage in these diseases, it is necessary to understand the signaling mechanisms that are involved in the activation of PMNs. In this report, we provided evidence that the release of ATP and autocrine purinergic signaling are central to the activation of PMNs. We showed that agonists of FPR and other GPCRs, as well as of structurally unrelated receptors on PMNs, triggered the release of ATP, which facilitated downstream signaling events that were required for the activation of functional cell responses. Purinergic signaling processes thus represent potential targets for therapeutic approaches to modulate the responses of PMNs in inflammatory or infectious diseases.

One such therapeutic approach could be to block the release of ATP. Although membrane-localized transporters, such as connexin and pannexin hemichannels, TTYH maxi-anion channels, and vesicular transport are implicated in the release of ATP from mammalian cells (15, 17, 2633), a clear understanding of which of these mechanisms facilitates the release of ATP from human PMNs in response to cell stimulation has been lacking. Some studies have shown that PMNs release ATP through Cx43 hemichannels (14). Here, we showed that human PMNs released ATP through TTYH3 maxi-anion channels and panx1 hemichannels, which are also implicated in the release of ATP from human T cells (16). Although TTYH3 maxi-anion channels and panx1 hemichannels release ATP, we found that only ATP that was released from panx1 hemichannels facilitated the functional responses of the cells that we investigated. Thus, the blockade of panx1 hemichannels may be a possible strategy to intercept purinergic signaling and to inhibit the activation of PMNs in inflammatory diseases. This notion is supported by reports that CBX, an inhibitor of panx1, prevents allergic airway inflammation in a mouse model of asthma (34).

GPCRs can form dimeric structures or higher-order oligomeric complexes that modulate the diverse biological responses elicited by these receptors (35). In addition to homomeric structures, GPCRs can also form heterodimers with unrelated GPCRs. Heterodimerization results in agonist specificities that seem to modify receptor functions (36). A number of purinergic receptor subtypes are thought to form such heterodimers either with other purinergic receptor subtypes (for example, A1 adenosine receptors with P2Y1 receptors) or with unrelated GPCRs (for example, A2a adenosine receptors with D2 dopamine receptors) (37, 38). Our findings showed that FPR and P2Y2 colocalized closely on the surface of PMNs, suggesting that they might form heteromeric complexes that associate with panx1 and thus could amplify FPR-induced signaling through purinergic autocrine feedback loops.

Extracellular nucleotides (such as ATP and its hydrolytic products) and purinergic receptors regulate a number of physiological processes, such as chloride secretion by epithelial cells, the redistribution of blood flow, and neurotransmission (39). Released ATP and other nucleotides activate P2 receptors that control cell functions that are associated with these physiological processes. Several studies reported that the activation of P2Y2 is involved in the production of IL-8 by retinal pigment epithelium cells and in the clearance of apoptotic cells by phagocytes (40, 41). Here, we showed that P2Y2 proteins formed a critical link in the signaling process that resulted in the activation of PMNs by infectious or inflammatory mediators. Our findings indicate that, although such inflammatory mediators induce certain signaling responses (such as the activation of ERK) in the absence of purinergic signaling, the initiation of effective functional responses in PMNs cannot occur without the release of ATP and autocrine purinergic feedback. Thus, to respond to specific extracellular cues, PMNs require both (i) specialized receptors that detect inflammatory or infectious mediators, and (ii) purinergic receptors that define and regulate the functional responses to such mediators.

Materials and Methods

Reagents and expression constructs

Apyrase, DIDS, CBX, human immunoglobulin G1 (IgG1-κ) antibodies, and dextran were from Sigma-Aldrich, and suramin was from Calbiochem. Percoll was obtained from Pharmacia. 10panx1 was from Tocris Bioscience and the panx1 control peptide (23) was from AnaSpec Inc. The mammalian expression vectors pEYFP-N1 and pEGFP-N1 were obtained from Clontech Laboratories. Expression vectors encoding fluorescent fusion proteins of human FPR1 and TTYH3 were generated in our laboratory from an FPR1-encoding plasmid obtained from Missouri S&T cDNA Resource Center and a hTTYH3 plasmid purchased from Thermo Fisher Scientific, Open Biosystems. All DNA constructs were confirmed by sequencing. The pECFP-P2Y2 receptor construct was a gift from H. Sitte and C. Nanoff (Medical University of Vienna).

Isolation and treatment of human PMNs

All studies were approved by the Institutional Review Board of the Beth Israel Deaconess Medical Center. PMNs were isolated from the peripheral blood of healthy volunteers as described previously (42). Before stimulation, PMNs were pretreated with different concentrations of DIDS, suramin, 10panx1, or apyrase for 10 min, unless indicated otherwise. These treatments did not change the viability of PMNs as determined by trypan blue dye exclusion.

Chemotaxis assays and measurements of MAPK activity

Chemotaxis assays and assays of the activity of MAPKs were performed as described previously (12, 42). PMNs were stimulated with 100 nM fMLP for 1 min in the case of MAPK assays or with 1 nM fMLP for 50 min for chemotaxis assays, and functional cell responses were determined.

Immunofluorescence staining

Human PMNs (2.5 × 106/ml) were plated on flamed 25-mm glass coverslips for 10 min at room temperature. All subsequent steps were performed at room temperature. The cells were fixed for 15 min with 3.7% paraformaldehyde in Hanks’ balanced salt solution (HBSS, Irvine Scientific). Cells were rinsed with HBSS and then permeabilized for 1 min with HBSS containing 0.01% Triton X-100 and blocked for 60 min with 5% human serum. The cells were incubated for 1 hour with rabbit antibody against hTTYH3 (1:200), goat antibody against human panx1 (1:200), or mouse antibody against human FPR (1:200). Cells were then incubated for 30 min in the dark with the appropriate secondary antibodies (1:1000): Alexa Fluor 555–conjugated goat antibody against rabbit IgG for hTTYH3, Alexa Fluor 594–conjugated rabbit antibody against goat IgG for panx1, and Alexa Fluor 488–conjugated goat antibody against mouse IgG for FPR. F-actin was stained with phalloidin (5 U per slide, Invitrogen). Fluorescence and bright-field images were acquired with a Leica DM-IRB fluorescence microscope. Control cells were treated identically except that incubation with primary antibodies was omitted. The presence of TTYH1 and Cx43 in human PMNs was examined by staining with rabbit antibody against hTTYH1 (1:200) or with rabbit antibody against human Cx43 (1:200). Antibody against human Cx43 was purchased from Cell Signaling Technology and antibodies against hTTYH1 and hTTYH3 were gifts of M. Suzuki (Jichi Medical School, Tochigi, Japan), who has demonstrated that these antibodies only recognize the respective human TTYH protein isoforms (15). Antibody against FPR was from BD Pharmingen and antibody against panx1 was from Santa Cruz Biotechnology; the selectivities of these antibodies were verified by their manufacturers.

Phagocytosis assays

An Alexa Fluor 488–labeled preparation of Escherichia coli was purchased from Invitrogen. Bacteria were opsonized by incubating equal volumes of 10% human serum and suspended bacteria (20 mg/ml) for 1 hour at 37°C. After two washes in HBSS, bacteria were incubated with PMNs at a ratio of 10:1 at 37°C for 30 min. Reactions were stopped by addition of ice-cold 1% formaldehyde in HBSS, and the cells were washed with 1% formaldehyde in HBSS. Uptake of bacteria was analyzed by flow cytometry according to the manufacturer’s guidelines.

Oxidative burst and degranulation assays

Oxidative burst was measured with dihydrorhodamine 123 (DHR; Invitrogen). Isolated PMNs were incubated with DHR (100 μM) and fMLP (100 nM) for 20 min and then placed on ice for 10 min to stop the reactions. Degranulation of PMNs was assessed by measuring the abundance of CD11b on the cell surface. PMNs were stimulated with fMLP (100 nM) for 10 min, chilled on ice, stained for 20 min each with monoclonal antibodies against CD11b/Mac-1 (BD Pharmingen) and phycoerythrin (PE)–conjugated horse antibody against mouse IgG (Sigma). Oxidative burst and degranulation were analyzed by flow cytometry with a BD FACSCalibur flow cytometer (Becton-Dickinson). To assess the abundance of CD11b on the surface of mouse PMNs, we diluted 100 μl of mouse whole blood with 100 μl of HBSS and incubated the blood for 20 min on ice and in the dark with fluorescein isothiocyanate–conjugated antibody against CD11b and PE-conjugated antibody against Gr-1 (both from Invitrogen and used at 1:200 dilution). Red blood cells were lysed for 4 min on ice with RBC Lysis Buffer (eBioscience) and the remaining cells were washed twice with HBSS, fixed with sheath fluid containing 0.5% formaldehyde, and analyzed by flow cytometry.

Cell culture and transfections

HL-60 cells were maintained and transfected with the pECFP-P2Y2 and pEYFP-FPR plasmids by electroporation as described previously (12). Briefly, cells were electroporated with 20 μg of plasmid per 2 × 106 cells with an Eppendorf Multiporator system set to 780 V, 300 μs, and 1 pulse or with 0.5 μg of plasmid per 5 × 105 cells with a Neon Transfection system (Invitrogen) set to 1350 V, 35 ms, and 1 pulse, according to the manufacturers’ protocols.

Measurement of ATP

Freshly isolated PMNs (2 × 106/ml) were treated with different concentrations of DIDS or 10panx1 for 10 min, stimulated with fMLP (100 nM) for 3 min or with human IgG1 for 10 min, placed on ice, and centrifuged at 325g for 1 min in the cold. The supernatants were treated as previously described (12) and the release of ATP was evaluated by measuring the concentrations of ATP in the supernatants with an ATP Bioluminescence Assay HS II Kit (Roche) and a Luminoskan plate luminometer (Labsystems) according to the manufacturer’s instructions or by high-performance liquid chromatography as previously described (12).

Real-time RT-PCR

The relative abundance of mRNAs for hTTYH1, hTTYH3, Cx43, and panx1 in human PMNs, undifferentiated HL-60 cells, and HL-60 cells differentiated for 3 days with 1.3% dimethyl sulfoxide (DMSO; dHL-60 cells) was determined by real-time RT-PCR analysis, as described previously (12), except that an Eppendorf Mastercycler Realplex real-time PCR system was used. Human brain complementary DNA (cDNA; BioChain Inc.) was used as a positive control. Predesigned QuantiTect primers were purchased from Qiagen. The supplier validated the primer sets bioinformatically and optimized them for use in real-time RT-PCR assays with SYBR Green. After performing real-time PCR analysis, we verified the correct PCR product sizes by agarose gel electrophoresis. The comparative Ct method was used for the relative quantification of gene expression as described previously (12). The abundance of each mRNA was normalized against that of β-actin.

Confocal microscopy

The presence of fluorescently labeled receptors in HL-60 cells was examined 24 hours after electroporation. Cells (2.5 × 106/ml) were plated on 25-mm glass-bottom dishes (MatTek) coated with human fibronectin (50 μg/ml; Sigma), and ECFP- and EYFP-labeled P2Y2 and FPR fusion proteins were imaged with a Zeiss LSM 510 Meta confocal microscope configured to excite both fluorescent proteins with multitrack mode with the 458- and the 514-nm laser lines of an argon laser source. The images in fig. S4 were recorded with an Ultraview VoX spinning disk confocal system from Perkin Elmer with solid-state diode laser sources emitting light at 442 and 515 nm.

Measurement of intracellular Ca2+

PMNs or HL-60 cells were loaded according to the manufacturer’s instructions with Fura-2-AM or Fluo-3-AM, respectively (Molecular Probes). Cells were stimulated with fMLP (10 nM). Changes in intracellular Ca2+ concentrations of cells loaded with Fura-2 were measured with a Kontron SFM 25 spectrofluorometer (Kontron Instruments). Ca2+ mobilization in HL-60 cells loaded according to the manufacturer’s suggestions with Fluo-3 in the presence of Pluronic (Molecular Probes) was analyzed by flow cytometry. HL-60 cells were gated to exclude debris or cell aggregates from the analysis. Cell responses were normalized with ionomycin (5 μM) to account for differences in the loading of Fluo-3 between individual cell preparations. Data were expressed as the percentage of the maximal Ca2+ response to that of the ionomycin-treated control.

Knockdown of P2Y2 and TTYH3

Six different siRNA constructs (Ambion) that targeted P2Y2 (siRNA IDs: 4419, 143690, 4237, 143692, 143691, and 4331) and three different siRNA constructs (Invitrogen) that targeted TTYH3 (cat. nos. HSS129677, HSS129678, and HSS129679) were tested. An unlabeled nonsense siRNA (Qiagen) was used as a negative control. The knockdown efficiency of each siRNA was initially tested in human embryonic kidney 293 cells (American Type Culture Collection) that were cotransfected with siRNA constructs and EGFP-P2Y2 or EGFP-TTYH3 expression plasmids with Lipofectamine 2000 (Invitrogen) according to the manufacturer’s instructions. Cells were harvested 24 hours later, and EGFP fluorescence was analyzed by flow cytometry. The siRNA constructs most effective in silencing EGFP-P2Y2 or EGFP-TTYH3 were selected (siRNA ID 4237 from Ambion for P2Y2 and siRNA cat. no. HSS129677 from Invitrogen for TTYH3). To verify the selectivity of knockdown experiments, we included a nonsense control siRNA construct in every experiment (fig. S4B). For silencing, HL-60 cells were transfected with 400 nM of each siRNA construct with the electroporation protocol and Eppendorf Multiporator system, as described earlier. Knockdown of P2Y2 or TTYH3 in HL-60 cells was assessed by determining the relative abundance of mRNAs by real-time RT-PCR, as described above.

Mouse model of infection

A mouse model of infection was established by performing cecal ligation and puncture (CLP) as described previously (5). C57BL/6J wild-type control mice were from the Jackson Laboratory and P2Y2 KO mice were a gift from R. Boucher (University of North Carolina, Chapel Hill, NC). These animals were backcrossed to a C57BL/6J genetic background for a total of 10 generations (backcrossed animals were provided by V. Vallon, University of California, San Diego, CA). For bacterial culture experiments, animals were euthanized after 3 hours and peritoneal lavage fluid (3 ml), heparinized blood (1 ml), livers, spleens, and lungs were collected. Each organ was homogenized in a total of 1 ml of sterile normal saline and 10-μl aliquots were plated onto trypticase soy agar plates (Becton-Dickinson) and cultured for 24 hours at 37°C, and colonies were counted. For CD11b experiments, animals were euthanized 2 hours after CLP and blood was collected, incubated with antibody against CD11b, and analyzed by flow cytometry, as described earlier.

Statistical analysis

All values are expressed as means ± SD. Statistical analysis was performed with unpaired Student’s t test or one-way analysis of variance (ANOVA) for comparison of multiple groups. Differences between groups were considered statistically significant when P < 0.05.


Acknowledgments: We thank H. Sitte and C. Nanoff (Medical University of Vienna, Vienna, Austria) for providing the pECFP-P2Y2 receptor construct. Funding: This study was supported in part by a Shock Society/Nova Nordisk research grant for Early Career Investigators (Y.C.) and by NIH grants GM-51477, GM-60475, AI-072287, and AI-080582 and Congressionally Directed Medical Research Programs grant PR043034 (W.G.J.). Author contributions: Y.C. performed most of the experiments and prepared the manuscript and figures; Y.Y. and U.K.T. provided technical and logistical assistance; Y.S., T.W., Y.I., and A.E. performed the animal experiments; A.L. and Q.Z. performed calcium measurements; C.H. helped with the discussion and interpretation of results; and W.G.J. was responsible for the design and coordination of the study and finalized the manuscript. Competing interests: The authors have no conflicts of interest to declare. Use of the expression plasmids described in this study requires a materials transfer agreement.

Supplementary Materials

Fig. S1. Colocalization of FPR and TTYH3 in human PMNs.

Fig. S2. Effects of blockers of ATP release on the ability of PMNs to hydrolyze extracellular ATP.

Fig. S3. Effects of blockers of ATP release on ATP-induced Ca2+ mobilization.

Fig. S4. Knockdown of P2Y2 and TTYH3.

Fig. S5. Colocalization of P2Y2 and FPR.

Movie S1. Z-stack view of a dHL-60 cell cotransfected with plasmids encoding P2Y2-ECFP (green) and FPR-EYFP (red).

Movie S2. A 3D view of a dHL-60 cell cotransfected with plasmids encoding P2Y2-ECFP (green) and FPR-EYFP (red).


References and Notes

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