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Institute of Molecular Physiology, University of Sheffield, Sheffield, United Kingdom
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Abstract |
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-NAD (1 mM) (but not any other nucleotide analogs tested). The results suggest that prolonged depolarization leads to an increased intracellular level of ADP-ribose, which in turn activates this nonselective conductance(s). |
Introduction |
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TopAbstractIntroductionMaterials and MethodsResultsDiscussionReferences |
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Although intracellular calcium plays a key role in several aspects of macrophage function, including activation, migration, and proliferation as well as generation of superoxide anion and stimulation of NO production, calcium influx is not immediately required for phagocytosis (4, 5, 6). It is unlikely that the well-studied store-operated or capacitative calcium entry current, which is present in all nonexcitable cells, could underlie the current associated with phagocytosis in macrophage because it shows a characteristically strong rectification, the currents are very small (only a few pA at -60 mV), and it is relatively impermeable to sodium under normal conditions (6, 7, 8, 9, 10, 11). Recently, a current has been described in the human macrophage U937 cell line that is activated by extracellular H2O2, or intracellular -NAD free acid (NAD+;3 1 mM) (12, 13) and might therefore underlie the current following phagocytosis described by Holevinsky and Nelson (1). This current is also activated by intracellular ADP-ribose at concentrations (10–300 µM) lower than those required for NAD+. It corresponds in some of its properties to the currents observed with heterologous expression of TRPM2 subunits (formerly called LTRPC2; for nomenclature, see Ref.14) (12, 13, 15).
These results are consistent with the interpretation that the prolonged depolarization that follows phagocytosis described by Holevinsky and Nelson (1) results from an inward current, such as that activated by NAD+ in U937 cells (12, 13). However, during the course of voltage-clamp recordings from rat peritoneal macrophages, we noticed that a sustained inward current could actually be activated by prolonged depolarization. In this work, we describe some properties of this current, and compare these with the current activated by NAD+ and ADP-ribose in the same cells. Both currents showed the same permeability to sodium, calcium, N-methyl-D-glucamine (NMDG), chloride, and gluconate ions, and sensitivity to block by lanthanum. The current activated by intracellular ADP-ribose occluded the depolarization-activated current. Thus, we conclude it is likely that these two stimuli activate the same conductance.
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Materials and Methods |
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Rat peritoneal cells were obtained from male Wistar rats (10 wk old) killed by cervical dislocation. The peritoneal cavity was lavaged with PBS (Life Technologies Cell Culture, Invitrogen, Paisley, U.K.). After centrifugation, the macrophage fraction was separated from the mast cells by fluorescence-activated cell sorting. Two populations of cells were separated by forward and side scatter. Cells were then collected by centrifugation and resuspended in DMEM (Life Technologies Cell Culture) containing 10% (v/v) FCS (Sigma-Aldrich, Poole, U.K.), 1% glutamine (Calbiochem, La Jolla, CA), and 1% antibiotics (Life Technologies Cell Culture, Invitrogen). Cells were plated onto glass coverslips and kept at 37°C in a humidified atmosphere containing 5% CO2. The cultured macrophages were used in patch-clamp experiments 1–3 days after plating. Cells were identified as macrophages using immunohistochemistry staining with the macrophage specifics Abs ED1–10 and ED-2 (Serotec, Oxford, U.K.).
HEK293 cells expressing P2X2/3 receptors
HEK293 cells were transfected, as previously described (16). Briefly, cells were electroporated (Gene Pulser; Bio-Rad, Hercules, CA) in the presence of 30 mg of plasmid containing both P2X2 and P2X3 receptor cDNAs. Following electroporation, cells were plated and selected for neomycin resistance, subcloned by FACS sorting, and resuspended in standard growth medium (Dulbecco’s) supplemented with 10% heat-inactivated FCS and 2 mM L-glutamine. Cells were grown to confluency and plated on coverslips, and recordings were made 2–48 h later.
Whole cell recording
Ion currents were studied using the whole cell configuration of the patch-clamp technique, as described by Hamill et al. (17). Glass electrodes (Harvard Apparatus, Edenbridge, U.K.) ranged from 6 to 8 M
in resistance and were fire polished. The indifferent electrode was an Ag-AgCl electrode connected to the bath through a short 3 M KCl agar bridge. All the experiments were performed at room temperature using an EPC9 patch-clamp system (HEKA, Lambrecht, Germany). The cells were kept in an extracellular solution containing (mM): NaCl, 147; KCl, 2; MgCl2, 1; CaCl2, 2; HEPES, 10; and glucose, 13. The pH was adjusted to 7.3 by adding NaOH (4 mM). The standard intracellular solution contained (mM): NaCl, 148; HEPES, 10; EGTA, 10. We used intracellular sodium rather than potassium in most experiments so that voltage-dependent potassium currents did not complicate our estimates of reversal potential. We used a high EGTA concentration so as to reduce any involvement of store-operated conductances in those cases in which we had calcium-free extracellular solutions. The pH was adjusted to 7.3 by adding NaOH (24 mM). Drug application and solution exchanges were conducted using a fast flow RSC 200 system (Biologic Science Instruments, Claix, France). Cells were held at -80 mV, except where stated, and current-voltage plots were obtained from ramp commands (-130 to 50 mV in 500 ms). Permeability experiments were conducted using standard intracellular solution and extracellular solution of different composition. The low NaCl solution contained (mM): NaCl, 40; HEPES, 10; CaCl2, 0.3 mM; glucose, 236 (pH brought to 7.3 with 4.2 mM NaOH). The NMDG solution contained (mM): NMDG, base 154; HEPES, 10; glucose, 23 (pH brought to 7.3 with HCl; final Cl concentration 146 mM). The gluconate solution contained (mM): Na-gluconate, 147; HEPES, 10; glucose, 33 (pH brought to 7.3 with 4 mM NaOH). The isotonic calcium solution contained (mM): CaCl2, 110; Ca(OH)2, 2; HEPES, 10; glucose, 12 (pH 7.3). Series resistance was compensated by 
75%.
Liquid junction potentials were calculated directly from ionic mobilities (18). Measured potentials were corrected for the junction potential existing at the recording pipette before seal formation (pipette solution -1.9 mV with respect to bath solution) and for any change in junction potential at the indifferent electrode when the bath solution was changed (<4 mV in all cases).
Intracellular sodium measurement
Cells were loaded with 1,3-benzenedicarboxylic acid, 4,4'-[1,4,10-trioxa-7,13-diazacyclopentadecane-7,13-diylbis(5-methoxy-6,2-benzofurandiyl)]bis-, tetra-ammonium salt (SBFI, 10 mM; Molecular Probes, Eugene, OR), and 0.02% pluronic acid for 45 min at 37°C. Ratiometric fluorescence measurements were performed using an Axiovert 100 microscope (Zeiss, Oberkochen, Germany). Cells were excited at 340 and 380 nm using a computer-driven monochromator, and the emission fluorescence (510 nm) was collected through a bandpass filter onto a charge-coupled device camera. Data were analyzed with Photonics software (Planegg, Germany).
Measurements of permeability
We first measured the permeability of chloride relative to that of sodium (PCl/PNa) in bi-ionic conditions. PCl/PNa was then calculated from PCl/PNa = ((1 - exp(-x)) x ([Na]o - [Na]i exp(x)))/(([Cl]i exp(-x) - [Cl]o) x (1 - exp(x))) (equation 1), where x = Er F/RT (extracellular 0.3 mM calcium ignored), where Er is the reversal potential, R is the Gas constant, F is the Faraday, and T is the absolute temperature. We used this value of PCl/PNa in subsequent calculations in which three permeant ions were present. The expressions used were: PNMDG/PNa = ((([Na]i exp(x) - [Na]o)/(1 - exp(x))) + PCl/PNa x (([Cl]i exp(-x) - [Cl]o)/(1 - exp(-x))))/(([NMDG]o - [NMDG]i exp(x))/(1 - exp(x))) (equation 2); Pgluc/PNa = ((([Na]i exp(x) - [Na]o)/(1 - exp(x))) + PCl/PNa x (([Cl]i exp(-x) - [Cl]o)/(1 - exp(-x))))/(([gluconate]o - [gluconate]i exp(-x))/(1 - exp(-x))) (equation 3); and PCa/PNa = (([Na]i exp(x)/(1 - exp(x))) - PCl/PNa x (([Cl]o - [Cl]iexp(-x))/(1 - exp(-x))))/(4 [Ca]o/(1 - exp(2x)) (equation 4). Although not shown in these equations, we have multiplied ion concentrations by the following activity coefficients: Na+, 0.8; K+, 0.8; Cl-, 0.8; NMDG+, 0.8; gluconate-, 0.8; Ca2+, 0.28 (19).
Data analysis
The results shown in the figures are mean ± SEM. Curve fits of the pooled data were performed using Kaleidagraph (Synergy Software, Reading, PA) and Excel (Microsoft, Redmond, WA) software. The lanthanum inhibition curve was fitted with I/Imax = 100 (IC50n/(IC50n + [La]n)), where I is the current at a given lanthanum concentration expressed as percentage of the current in the absence of lanthanum (Imax), IC50 is the lanthanum concentration at which I = 0.5 x Imax, and n is the Hill coefficient. Concentration-current curves were fitted with I/Imax = 100 ([ADP-ribose]n/([ADP-ribose]n + EC50n)), where I is the current activated by a given concentration of ADP-ribose and expressed as percentage of the maximal currents (Imax), EC50 is the ADP-ribose concentration evoking half of the maximal current, and n is the Hill coefficient.
Chemicals
ADP, ADP-glucose, ADP-ribose, cyclic ADP-ribose, AMP, ATP, EGTA, lanthanum chloride, D-ribose, D-ribose 5-phosphate, NMDG, xanthine, and xanthine oxidase were purchased from Sigma-Aldrich. NAD+, -NAD disodium salt (NADH), -NAD phosphate disodium salt (NADP+), -NADPH disodium salt (NADPH), and 1-[b-[3-(4-methoxyphenyl)propoxy]-4-methoxyphenethyl]-1H-imidazole (hydrochloride; SKF96365) were purchased from Calbiochem. SBFI was from Molecular Probes.
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Results |
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Current activated by depolarization
Cells held at -80 mV showed no change in holding current or conductance during 5–10 min of whole cell recording. However, if the cell was held at +10 mV for several tens of seconds and then returned to -80 mV, a large inward current was observed (Fig. 1A). This current quickly (<5 s) reached its peak amplitude (several hundred pA) and then declined during the next few minutes (Fig. 1A; in 10 cells the amplitude after 2 min was 19 ± 4% of the peak amplitude). The duration of the depolarization required to evoke the subsequent inward current was not studied in detail; however, a depolarization to +10 mV for only 10 s was not effective (n = 5). After an interval of several minutes, a second depolarization again elicited a large inward current with similar properties (n = 10).
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0.5 (Table I). When extracellular sodium was substituted by NMDG, the current evoked by depolarization was reduced to 79 ± 2% (n = 6) of its control value (measured at -80 mV). The residual current reversed polarity at -5.4 ± 0.45 mV (n = 7) (Table I; Fig. 2A), which indicates that NMDG is significantly permeable (PNMDG/PNa 0.74; from equation 2). When extracellular gluconate replaced chloride, the current at -80 mV was reduced to 91 ± 4% (n = 4), and when extracellular calcium replaced sodium, the inhibition was to 48 ± 6% (n = 6) of control (Fig. 2B). By measuring the reversal potential of the residual current (Table I), it was evident that the conductance activated by prolonged depolarization is significantly permeable to chloride and gluconate, NMDG, and calcium ions. In each of these ion substitutions, the current-voltage relation remained essentially linear (Fig. 2).
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meATP (30 µM) to activate the inward current in cells expressing P2X2/3 subunits, which was typically 1 nA in amplitude (20). We observed that the agonist-induced current reversed polarity at 0.8 ± 0.5 mV (n = 23) in control extracellular solution, -33 ± 1.4 mV (n = 4) in 40 mM NaCl, and -86.5 ± 0.4 mV (n = 4) in NMDG solution. These reversal potentials correspond (from equations 1 and 2) to relative permeabilities of PCl/PNa < 0.02 and PNMDG/PNa < 0.03 (see Ref.21).
The current induced by depolarization was substantially blocked by lanthanum (10 µM) (Fig. 1); the IC50 for this action was 1 µM (Fig. 3A). The current was also significantly inhibited (76 ± 10%, n = 4) by SKF96365 (100 µM); at 10 µM SKF96365 inhibited the current in some (75 ± 8%, n = 4), but not other (n = 3) cells. SKF96365 has been widely used to block nonselective cation channels and store-operated calcium entry in nonexcitable cells since its introduction by Merritt et al. (22). The current evoked by depolarization was also greatly reduced by including in the pipette either ATP (5 mM, inhibited by 89 ± 5%, n = 4) or ADP (10 mM, inhibited by 97 ± 4%, n = 5) (Fig. 3B).
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An inward current progressively developed over tens of seconds in cells held at -80 mV, when the recording electrode contained ADP-ribose (Fig. 4A). The current-voltage relation remained linear throughout this period, and reversed close to 0 mV (-2.7 ± 0.6 mV, n = 11) (Fig. 4B). With 1 µM ADP-ribose, the development of the current was fitted by an exponential with a time constant of 1 min (Fig. 4C). The lowest concentration of ADP-ribose that was effective was 100 nM, and maximum value of the current was reached with 100 µM; the EC50 was 10 µM (Fig. 4D). Changing the level of intracellular calcium buffering did not obviously alter the effectiveness of ADP-ribose to activate this current. In our control, strongly buffered solution (10 mM EGTA, 0 mM calcium, 1 nM [Ca]i) ADP-ribose (300 µM) elicited a current of 703 ± 119 pA (n = 3); with a higher level of intracellular calcium (11 mM EGTA, 2 mM calcium, 100 nM [Ca]i), this was 811 ± 149 pA (n = 5). No similar current developed when the recording electrode contained ADP (100 µM), ADP-glucose (100 µM), cyclic ADP-ribose (100 µM), AMP (100 µM), ATP magnesium salt (100 µM), D-ribose (100 µM), D-ribose 5-phosphate (100 µM), NADH (300 µM or 1 mM), NADP+ (300 µM), or NADPH (300 µM) (n = 3 cells in all cases). However, NAD+ at a concentration of 1 mM (n = 4) evoked a current similar to that observed with ADP-ribose, although 100 and 300 µM were ineffective. The peak current elicited by NAD+ (1 mM) was 758 ± 428 pA (n = 4), which is not different from that seen with ADP-ribose (Fig. 4).
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The current evoked by ADP-ribose was also very sensitive to block by extracellular lanthanum (Fig. 3A), with an IC50 of 10 µM. It was also blocked by SKF96365 (100 µM, 77 ± 4%, 5 of 5 cells tested; 10 µM, 70 ± 7%, 7 of 12 cells tested) and by intracellular either ATP (5 mM, inhibited by 66 ± 11%, n = 5) or ADP (10 mM, inhibited by 76 ± 3%, n = 4) (Fig. 3B). These relative inhibitions were not different from those observed for the current activated by depolarization (ANOVA, p > 0.05).
A membrane current with similar properties was also elicited by applying xanthine (0.1 mM) and xanthine oxidase (0.05 U/ml), to generate superoxide anions; this current was completely blocked by 100 µM lanthanum (Fig. 5A). Application of xanthine alone had no effect. In parallel experiments, we used intracellular sodium imaging as an index of depolarization of undisturbed macrophages. In these cells, H2O2 (10 mM) evoked a progressive increase in intracellular sodium concentration ([Na]i) (Fig. 5B). The time course of the [Na]i increase was similar to that of the inward current observed with xanthine/xanthine oxidase, or depolarization, and the increase in [Na]i was also strongly reduced by lanthanum (1 mM) (Fig. 5B).
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The similar properties of the two currents led us to hypothesize that sustained depolarization and intracellular ADP-ribose were activating the same conductance. We recorded from 10 cells with electrodes containing ADP-ribose (300 µM); after 4 min, when the inward current reached its steady value, we applied a depolarization to +10 mV for an additional 4 min. This depolarization evoked no additional current. In time-matched controls, the depolarization elicited large inward currents recorded at -80 mV (Fig. 6).
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Discussion |
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TopAbstractIntroductionMaterials and MethodsResultsDiscussionReferences |
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0.02). The estimates of permeability to NMDG, calcium, and gluconate should be considered as less reliable than those for PCl/PNa. This is because in those cases there are three permeant ions present, and the estimate involves using the value previously determined for PCl/PNa. Likewise, the reversal potential observed with extracellular NMDG indicates that the P2X2/3 receptor is essentially impermeant (PNMDG/PNa < 0.03), whereas both the currents presently studied in macrophages have significant permeability to NMDG. From experiments of the type described, it is difficult to exclude the possibility that the sustained depolarization is activating more than one set of ionic channels; for example, one permeable to anions and another permeable to cations. All that can be said in this case is that each has a very similar, and linear, current-voltage relation and each has a similar sensitivity to block by lanthanum. We shall return later to discuss the question of how a sustained depolarization might lead to the activation of such an ionic conductance(s).
There are many similarities between these permeation properties and those reported by Holevinsky and Nelson (1) for the current following phagocytosis of fluorescein-labeled immune complexes recorded from macrophages derived from human blood monocytes. That was a large current (typically 1 nA), similar in amplitude to the currents that we presently describe; this is in marked contrast to the very small (50 pA) current elicited by thapsigargin in the same cells (10). The underlying conductance had PNMDG/PNa of 0.69 in the work of Holevinsky and Nelson (1), which is close to our present estimate. Furthermore, they also reported that the underlying channels had significant anion permeability, and that glutamate appeared to be more permeable than chloride. That current was also completely blocked by 1 mM lanthanum, although the effects of lower concentrations were not examined. Holevinsky and Nelson (1) found that a current with similar properties could be activated by xanthine plus xanthine oxidase, although not by xanthine alone, and they suggested that the release of free radicals following phagocytosis activated the underlying conductance. Holevinsky and Nelson (1) did not investigate whether a sustained depolarization could elicit such a current, as we have reported; they did report that, under current clamp, the current led to a sustained depolarization of the cells.
It has recently become clear that oxidants such as H2O2 can indeed activate a cation conductance in certain immune cells (12). In the monocytic cell line U937, as well as Jurkat T lymphocytes and the eosinophil line EOL1, this can be mimicked by intracellular NAD+, but not by NADH (12, 13). This implies that NAD+, formed by the action of free radicals on intracellular NADH, mediates the effect. The molecular identity of the underlying channel has been approached in two ways. First, heterologous expression of TRPM2 cDNA results in the appearance of channels permeable to cations that can be activated by intracellular NAD+ (=1 mM) (12, 13). Second, treatment of U937 monocytes with antisense oligonucleotides that reduced the expression of TRPM2 (measured by Western blotting and immunocytochemistry) also reduced the calcium entry and cell death elicited by H2O2 (12). These experiments strongly suggest that one or more TRPM2 subunits are a key component of the channel expressed by these immune cell lines that is activated by oxidative damage (12, 13). In contrast, it has recently been found that H2O2 can activate heterologously expressed TRPM2 channels by a mechanism that appears not to involve changes in ADP-ribose or NAD levels (23).
The homomeric channels formed by expression of TRPM2 subunits are directly activated also by ADP-ribose (13, 15), although not by several closely related analogs (cyclic ADP-ribose, NADH, NADP+, NADPH, ATP, and ADP) (12, 13, 15). The activation results from binding of the ADP-ribose to a Nudix domain in the C terminus of the protein, because it is prevented by point mutations of key residues in this motif (12, 15). The concentration of ADP-ribose causing 50% activation of the whole cell current is 30–100 µM (15). When activated by intracellular diffusion of ADP-ribose during the course of whole cell recordings, these TRPM2 currents show close to linear I/V relations and others properties that resemble the current first described by Wilding et al. (24) in ascidian oocytes.
The current that we now report in rat peritoneal macrophages, which is activated by ADP-ribose, has some, but not all, of the same features. These include the effectiveness of ADP-ribose and NAD+ (although not a range of other structurally related compounds), the effective concentrations of ADP-ribose (EC50 30 µM; Fig. 4D) and NAD+ (1 mM), and the block by ATP (5 mM) (13). We considered that an excess of ADP might inhibit the binding of ADP-ribose to its Nudix domain (25), and consistent with this we observed that intracellular ADP also blocked the currents activated by both ADP-ribose and depolarization. However, there also appear to be important differences between the properties of heterologously expressed TRPM2 channels and the macrophage currents. The most notable is the significant permeability to NMDG, chloride, and gluconate that we observed, whereas substitution of external cations by NMDG almost completely blocks the current through homomeric TRPM2 channels (13, 15). Furthermore, we observed a relatively high sensitivity to lanthanum (IC50 
1–10 µM) on the depolarization-evoked and ADP-ribose-evoked current in peritoneal macrophages, but the sensitivity of TRPM2 currents to lanthanum has not yet been studied systematically.
In contrast, other currents have been described with properties that more closely resemble the macrophage currents observed in the present study. For example, heterologous expression of PKD1 and PKD2, genes named for the polycystic kidney disease that arises when they are mutated in humans (26), gives rise to a similar conductance (27). Those channels have PNMDG/PNa of 0.51. The PCl/PNa cannot be calculated directly from the data of Hanaoka et al. (27) (they had three permeant ions present: cesium, sodium, and chloride); however, the 45 mV shift in reversal potential would indicate PCl/PNa of 0.3. The lanthanum sensitivity of the PKD1/2 current (50% inhibition by 50 µM) is also not very different from that which we observed in peritoneal macrophages. It is not clear how polycystin channels could be activated by NAD+ and ADP-ribose, because their amino acid sequence does not contain a Nudix domain. Further work, such as recordings of single channel activity and antisense oligonucleotide approaches, will be needed to establish the molecular composition of the macrophage channel.
The occlusion experiment illustrated in Fig. 5 strongly suggests that the two currents that we describe pass through the same channels (although it is also formally possible that intracellular ADP-ribose could in some way inhibit the effect of depolarization to activate a separate population of channels). This is consistent with the overall similarity in the properties of the currents with respect to permeability (Table I) and lanthanum blockade (Fig. 3). This raises the question deferred earlier: what might be the mechanism by which sustained depolarization activates this cell conductance? Speculations might include that depolarization evokes the release of ADP-ribose from intracellular stores, or in some way facilitates its synthesis from NAD+. In the latter regard, it is worth noting that the enzyme responsible for the formation of ADP-ribose from NAD+ (CD38, NAD-glycohydrolase) is itself membrane associated, with its enzymatic activity in the ectodomain (28, 29). It is possible that the movement of negatively charged ADP-ribose into the cell is in some way facilitated by the sustained applied depolarization. Our observation that the current elicited by depolarization and the current evoked by intracellular ADP-ribose had very similar sensitivities to blockade by intracellular ATP and ADP (Fig. 3B) is obviously consistent with the interpretation that ADP-ribose serves as the messenger for the depolarization. In this case, as with the experiments using xanthine and xanthine oxidase, it must be argued the involvement of ADP-ribose is local rather than distributed throughout the cytoplasm; this is because the responses were well maintained in cells during relatively long periods of intracellular dialysis with the contents of the recording pipette.
In conclusion, an imposed depolarization of macrophages activates an inward current that is significantly permeable to large cations as well as anions, and that is blocked by low µM concentrations of lanthanum. Under more physiological circumstances (i.e., without voltage-clamp), this current could amplify the depolarization by opening further channels. In this way, the effect of an initial stimulus that leads to the release of free radicals within the cell (such as phagocytosis) would be further enhanced. Such a positive feedback process, in which activation of the current leads to depolarization of the macrophage and depolarization leads to further activation, might contribute to the eventual cell death that readily follows exposure to exogenous oxidants.
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Acknowledgments |
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Footnotes |
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2 Address correspondence and reprint requests to Dr. R. Alan North, Institute of Molecular Physiology, Alfred Denny Building, Western Bank, University of Sheffield, Sheffield S10 2TN, U.K. E-mail address: r.a.north{at}sheffield.ac.uk
3 Abbreviations used in this paper: NAD+, -NAD free acid; NADH, -NAD disodium salt; NADP+, -NAD phosphate disodium salt; NADPH, -NADPH disodium salt; NMDG, (N-methyl-D-glucamine); SBFI, 1,3-benzenedicarboxylic acid, 4,4'-[1,4,10-trioxa-7,13-diazacyclopentadecane-7,13-diylbis(5-methoxy-6,2-benzofurandiyl)]bis-, tetra-ammonium salt; SKF96365, (1-[b-[3-(4-methoxyphenyl)propoxy]-4-methoxyphenethyl]-1H-imidazole hydrochloride.
Received for publication July 9, 2002. Accepted for publication November 18, 2002.
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References |
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receptor-initiated phagocytosis. J. Biol. Chem. 270:22301.This article has been cited by other articles:
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  E. F. Vernon-Wilson, F. Aurade, L. Tian, I. C. M. Rowe, M. J. Shipston, J. Savill, and S. B. Brown CD31 delays phagocyte membrane repolarization to promote efficient binding of apoptotic cells J. Leukoc. Biol., November 1, 2007; 82(5): 1278 - 1288. [Abstract] [Full Text] [PDF]
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 T. Schilling, F. Lehmann, B. Ruckert, and C. Eder Physiological mechanisms of lysophosphatidylcholine-induced de-ramification of murine microglia J. Physiol., May 15, 2004; 557(1): 105 - 120. [Abstract] [Full Text] [PDF]
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 A. B. Mackenzie, H. Chirakkal, and R. A. North Kv1.3 potassium channels in human alveolar macrophages Am J Physiol Lung Cell Mol Physiol, October 1, 2003; 285(4): L862 - L868. [Abstract] [Full Text] [PDF]
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), and did not occur with a holding potential of -80 mV (
). Points are mean amplitude (±SEM) for eight (+10 mV), three (-40 mV), and five (-80 mV) cells.
, 1 µM (n = 3); 
, 100 µM (n = 6); and 
, 300 µM (n = 6). The currents are normalized to the value at 240 s in each particular cell; these values were 66 ± 25 pA (4), 309 ± 143 pA (6), 356 ± 145 pA (3), 949 ± 390 pA (6), and 1521 ± 432 pA (6) for control, 100 nM, 1 µM, 100 µM, and 300 µM, respectively. The numbers beside each trace are the time constants of fitted exponentials. Holding potential -80 mV. D, Concentration-response curve for current measured at 240 s as a function of intracellular ADP-ribose concentration (n = 3–6 cells for each point).
