Basic Research

Slit2 Prevents Neutrophil Recruitment and Renal Ischemia-Reperfusion Injury

Swasti Chaturvedi, Darren A. Yuen, Amandeep Bajwa, Yi-Wei Huang, Christiane Sokollik, Liping Huang, Grace Y. Lam, Soumitra Tole, Guang-Ying Liu, Jerry Pan, Lauren Chan, Yaro Sokolskyy, Manoj Puthia, Gabriela Godaly, Rohan John, Changsen Wang, Warren L. Lee, John H. Brumell, Mark D. Okusa and Lisa A. Robinson
JASN August 2013, 24 (8) 1274-1287; DOI: https://doi.org/10.1681/ASN.2012090890

Abstract

Neutrophils recruited to the postischemic kidney contribute to the pathogenesis of ischemia-reperfusion injury (IRI), which is the most common cause of renal failure among hospitalized patients. The Slit family of secreted proteins inhibits chemotaxis of leukocytes by preventing activation of Rho-family GTPases, suggesting that members of this family might modulate the recruitment of neutrophils and the resulting IRI. Here, in static and microfluidic shear assays, Slit2 inhibited multiple steps required for the infiltration of neutrophils into tissue. Specifically, Slit2 blocked the capture and firm adhesion of human neutrophils to inflamed vascular endothelial barriers as well as their subsequent transmigration. To examine whether these observations were relevant to renal IRI, we administered Slit2 to mice before bilateral clamping of the renal pedicles. Assessed at 18 hours after reperfusion, Slit2 significantly inhibited renal tubular necrosis, neutrophil and macrophage infiltration, and rise in plasma creatinine. In vitro, Slit2 did not impair the protective functions of neutrophils, including phagocytosis and superoxide production, and did not inhibit neutrophils from killing the extracellular pathogen Staphylococcus aureus. In vivo, administration of Slit2 did not attenuate neutrophil recruitment or bacterial clearance in mice with ascending Escherichia coli urinary tract infections and did not increase the bacterial load in the livers of mice infected with the intracellular pathogen Listeria monocytogenes. Collectively, these results suggest that Slit2 may hold promise as a strategy to combat renal IRI without compromising the protective innate immune response.

AKI develops in 5% of hospitalized patients and leads to significant morbidity, mortality, and financial costs.1–3 Fifty percent of AKI cases result from ischemia-reperfusion injury (IRI).4 Despite significant advances in the understanding of kidney IRI pathogenesis, specific therapy remains elusive, and management is mainly supportive.5

IRI leads to the recruitment of circulating leukocytes, particularly neutrophils, into the injured kidney.6–9 After recruited, neutrophils exacerbate damage by releasing inflammatory mediators.10–12 Therapies targeting only single aspects of neutrophil recruitment are only partially effective in ameliorating renal injury.13,14 Given the diversity of neutrophil attractants and the involvement of other leukocyte subsets, it is unlikely that a single antichemotactic therapy will be entirely effective.15 A generalized strategy to inhibit recruitment of inflammatory leukocytes would be more beneficial.

The Slit family of secreted proteins and their receptor Roundabout (Robo) repel neurons during central nervous system development.16,17 Slit has three known isoforms (Slit1–3), and Robo has four isoforms (Robo-1 to -4).18 The persistent expression of Slit and Robo in the mature organism suggests biologic functions that extend beyond development.19 We and others have previously shown that Slit2 and Robo-1 inhibit chemotaxis of neutrophils, T lymphocytes, and dendritic cells to diverse chemoattractants.20–23 The role of Slit2 in modulating renal inflammation associated with AKI, however, has not been previously explored.

Here, we report that Slit2 potently inhibits multiple steps involved in recruitment of circulating neutrophils. In vivo, we show that Slit2 administration prevents tubular injury, neutrophil infiltration, and renal failure associated with postischemic AKI. We also show that Slit2 does not impair critical protective immune functions of neutrophils and does not increase susceptibility to bacterial infection. These results suggest that Slit2 represents a potential strategy for the prevention and treatment of AKI without compromising protective host innate immune functions.

Results

Endogenous Levels of Slit2 Decrease in the Kidney after IRI

To explore the role of Slit2 in IRI, we first examined endogenous renal Slit2 levels in a mouse model of bilateral kidney IRI that mimics clinical ischemic AKI.24–26 Although Slit2 protein was detected in the glomeruli and tubulointerstitium of sham-operated kidneys, a significant downregulation of Slit2 levels was noted after ischemia-reperfusion (Figure 1).

Figure 1.
Figure 1.

Slit2 protein levels decrease in the kidney after IRI. Representative images of frozen kidney sections immunofluorescently labeled with anti-Slit2 antibody and Alexa 488 anti-goat IgG (green) from mice subjected to (A–C) sham surgery and (D–F) IRI. Original magnification, ×20. (A and D) DiI-conjugated wheat germ agglutinin staining (red) was performed to delineate cell membranes. (B and E) Immunolabeled Slit2 (green) and (C and F) merged images. White arrows indicate interstitial Slit2 staining. (G) Quantitative analysis of Slit2 levels using Volocity software was performed on 10 random, nonoverlapping 20× cortical fields sampled from sham surgery (n=3) and IRI kidneys (n=6) immunofluorescently labeled for Slit2. Data are presented as mean ± SEM. *P<0.05 versus sham surgery kidneys.

Slit2 Inhibits Neutrophil Adhesion to Activated Endothelial Cells

We showed that neutrophils express the Slit2 receptor, Robo-1 (Supplemental Figure 1), and that Slit2 inhibits neutrophil chemotaxis to diverse chemoattractants by preventing activation of Rho-family guanosine triphosphatases (GTPases).22 The reduction in renal Slit2 after IRI suggested its potential involvement in regulating neutrophil recruitment. Because multiple steps in neutrophil recruitment are Rho-family GTPase-dependent, we established cell culture models to examine the effects of Slit2 on each step of neutrophil recruitment in the setting of IRI. We first tested the effects of Slit2 on adhesion of human neutrophils to human umbilical vein endothelial cells (HUVEC) stimulated by TNF-α, an inflammatory cytokine locally upregulated after IRI.27 Although neutrophils only minimally adhered to unstimulated HUVEC, their adhesion was enhanced after TNF-α activation of HUVEC (Figure 2A, P<0.05 versus control). In the presence of full-length human Slit2 (hSlit2), neutrophil adhesion decreased (Figure 2A, P<0.05 versus TNF-α–stimulated HUVEC).

Figure 2.
Figure 2.

Slit2 inhibits neutrophil adhesion to activated endothelial cells. Freshly isolated human neutrophils were labeled with calcein and incubated with PBS, full-length hSlit2, or the bioactive N-hSlit2. Neutrophils (105 cells/well) were incubated with confluent HUVEC monolayers and allowed to adhere for 30 minutes. Nonadherent cells were removed, and neutrophil adhesion was quantified using a fluorescent plate reader at excitation and emission wavelengths of 494 and 517 nm, respectively. (A) The effects of hSlit2 on neutrophil adhesion to HUVEC prestimulated with TNF-α. (B) To determine whether the observed effects of Slit2 result from its actions on neutrophils and/or endothelial cells, neutrophils were incubated with N-hSlit2 for 10 minutes, and unbound N-hSlit2 was washed away before performing the adhesion assays. In parallel experiments, endothelial cells were incubated with N-hSlit2, and unbound N-hSlit2 was washed away before performing the adhesion assays. (C) Hypoxic conditions were induced by exposing HUVEC to 1% oxygen at 37°C. Cells were exposed to 2 hours of hypoxia followed by the indicated periods of reoxygenation, and neutrophil adhesion assays were performed as in A. *P<0.05 versus basal. †P<0.05 versus TNF-α stimulation. ‡P<0.05 versus HUVEC exposed to 2 hours of hypoxia followed by 0.5 hours of reoxygenation. §P<0.05 versus HUVECs exposed to 2 hours of hypoxia followed by 3 hours of reoxygenation. Mean values ± SEM from three to five independent experiments.

To confirm the specificity of this inhibition, we used a bioactive N-terminal fragment of hSlit2 (N-hSlit2). N-hSlit2 inhibited neutrophil adhesion to endothelium activated by TNF-α (Figure 2B and Supplemental Figure 2, P<0.05 versus TNF-α–stimulated HUVEC). We also used a soluble truncated species of the Robo-1 receptor (RoboN), which acts as a decoy receptor for Slit2.28 Preincubation of N-hSlit2 with RoboN abrogated the effects of N-hSlit2 (Supplemental Figure 2), indicating that the inhibitory effects of Slit2 are Robo-1–dependent.

The observed effects of Slit2 on neutrophil adhesion could result from direct actions on neutrophils and/or HUVEC. HUVEC expressed Robo-1, -2, and -4, suggesting that these cells may also be Slit2-responsive (Supplemental Figure 3).29 To determine whether the observed effects of Slit2 result from its actions on neutrophils and/or endothelial cells, neutrophils were first incubated with N-hSlit2, after which unbound N-hSlit2 was washed away before performing the adhesion assays. When unbound Slit2 was removed, neutrophil adhesion was inhibited to the same extent as when Slit2 was present throughout the assay (Figure 2B). Conversely, when HUVEC were incubated with Slit2 and unbound Slit2 was then removed, neutrophil adhesion was not inhibited (Figure 2B). Collectively, these data show that Slit2 acts directly on neutrophils and not endothelial cells to impair neutrophil adhesion to injured endothelium.

Slit2 Inhibits Neutrophil Adhesion to Endothelial Cells Subjected to Hypoxic Injury

Although TNF-α is an important endothelial activator that is upregulated after IRI, it is only one of a number of such signals. We, therefore, examined the effect of Slit2 on neutrophil adhesion to endothelial cells exposed to hypoxia-reoxygenation (H/R), confirming first that H/R resulted in endothelial injury (Supplemental Figure 4).30 When HUVEC were exposed to 2 hours of hypoxia followed by 0.5 or 3 hours of reoxygenation, neutrophil adhesion increased (Figure 2C, P<0.05 versus control). Neutrophils preincubated with hSlit2 adhered less to HUVECs exposed to H/R after reoxygenation periods of both 0.5 and 3 hours (Figure 2C, P<0.05 hSlit2-treated versus untreated neutrophils).

Slit2 Reduces Neutrophil Capture by and Adhesion to Activated Endothelial Cells

The static adhesion assays described above test the effects of Slit2 on neutrophil adhesion in the absence of shear flow. To test steps upstream of firm neutrophil adhesion in a system more closely representative of the in vivo setting, we used a microfluidic system to examine neutrophil–endothelial interactions under shear flow conditions that mimic the renal microvasculature.31 Although only 8±1 neutrophils interacted with endothelium per high power field (hpf) under basal conditions after 1 minute of flow (Supplemental Video 1), the number of interacting neutrophils increased after HUVEC stimulation with TNF-α to 53±4 cells/hpf (Figure 3A and Supplemental Video 2, P<0.01 versus basal). In the presence of hSlit2, the number of rolling and adherent neutrophils interacting with activated endothelium was reduced (Figure 3A and Supplemental Video 3, P<0.05 TNF-α versus TNF-α + hSlit2). When Slit2 was preincubated with RoboN, its inhibitory effect was attenuated (Supplemental Figure 5 and Supplemental Video 4). Collectively, these data show that, under shear flow, Slit2 prevents the initial capture and adhesion of neutrophils to activated endothelium.

Figure 3.
Figure 3.

Slit2 inhibits neutrophil capture by, adhesion to, and transendothelial migration across activated endothelial cells under shear flow conditions. HUVEC grown to confluence in channels of the Bioflux microfluidic system were incubated with TNF-α for 4 hours. Calcein-labeled human neutrophils were preincubated with PBS or hSlit2 and then perfused through the channels at a shear rate of 0.5 dynes/cm2. A Nikon TE2000 inverted microscope and Hamamatsu video camera were used to video record neutrophil–HUVEC interactions. Neutrophil adhesion was quantified using Bioflux Montage software. (A) Neutrophil–endothelial interactions were recorded after 1 minute of flow at 0.5 dynes/cm2, and the number of neutrophils that were rolling and firmly arrested was determined. (B) Neutrophil adhesion to the endothelial monolayer was determined after 12 minutes of shear flow at 0.5 dynes/cm2, and representative images were taken from three to five independent experiments using a 20× objective. (C) Experiments were performed as in B, and the number of neutrophils was quantified. (D) To assess the effects of Slit2 on neutrophil transendothelial migration, HUVEC were grown to confluence on fibronectin-coated polyester transwell inserts placed in a 24-well plate and exposed to hypoxia (2 hours) followed by reoxygenation (0.5 hours). Calcein-labeled human neutrophils were incubated with PBS or Slit2 (4.5 µg/ml) for 10 minutes and placed in the upper well of the transwell chamber, and the chemokine IL-8 (50 ng/ml) was added to the lower well. Neutrophils were allowed to migrate for 3 hours at 37°C. Neutrophils that had migrated from the upper to the lower well were permeabilized with 1% Triton, and the fluorescence emitted was read using a fluorescent plate reader. Mean values ± SEM from three independent experiments. *P<0.05 versus TNF-α–stimulated HUVECs. †P<0.05 versus basal HUVEC. ‡P<0.05 versus IL-8 treatment and HUVEC exposure to 2 hours of hypoxia followed by 0.5 hours of reoxygenation.

These early effects also translated into a significant reduction in total neutrophil adhesion at later time points. After 12 minutes of shear flow, under basal conditions, there was minimal neutrophil adhesion to endothelium. Although activation of HUVEC with TNF-α increased neutrophil adhesion (P<0.05 versus basal), this adhesion was reduced by preincubating the neutrophils with Slit2 (Figure 3, B and C, P<0.05 versus TNF-α).

Slit2 Reduces Chemoattractant-Induced Neutrophil Transendothelial Migration

After neutrophils firmly adhere to the injured endothelium, they undergo Rho-family GTPase-dependent transmigration across the endothelial barrier to infiltrate the injured kidney in response to the local release of chemoattractants, such as IL-8.32–34 We tested the effect of Slit2 on IL-8–mediated transendothelial migration of neutrophils in the absence or presence of H/R injury. Although IL-8 increased neutrophil migration across uninjured or H/R-injured HUVEC monolayers (Figure 3D and Supplemental Figure 6, P<0.05 versus control), hSlit2 decreased neutrophil transendothelial migration to near basal values (Figure 3D and Supplemental Figure 6, P<0.05 versus IL-8).

Slit2 Prevents Renal IRI

Having shown that Slit2 inhibits multiple steps in neutrophil recruitment, we next examined the effect of Slit2 administration on mice subjected to renal IRI. After 18 hours, plasma creatinine was more than sevenfold higher in mice that underwent bilateral renal IRI compared with sham-treated mice (Figure 4A, P<0.05). hSlit2 administration prevented the rise in plasma creatinine in a dose-dependent manner (Figure 4A, vehicle versus Slit2 at 1 µg, P<0.05; vehicle versus Slit2 at 2 µg, P<0.05; Slit2 at 2 µg versus Slit2 at 1 µg, P<0.05). Administration of a bioactive N-terminal fragment of mouse Slit2 (N-mSlit2) also reduced plasma creatinine (Figure 4B, P<0.05), whereas preincubation of N-mSlit2 with RoboN attenuated this protective effect (Figure 4B).

Figure 4.
Figure 4.

Slit2 prevents renal dysfunction after IRI. (A) IRI was induced by bilateral cross-clamping of renal pedicles of male C57BL/6 mice for 26 minutes. Full-length hSlit2 (at the indicated doses) or vehicle was administered intraperitoneally before inducing IRI; 18 hours after reperfusion, blood was drawn by retro-orbital bleed, and plasma creatinine was determined using a colorimetric assay. (B) Truncated N-mSlit2 (2 µg) with or without molar equivalent amounts of RoboN was administered intraperitoneally before induction of renal IRI, and experiments were performed as in A. Mean values ± SEM from four to seven mice per experimental group. *P<0.05 versus sham-operated mice. †P<0.05 versus vehicle-treated IRI mice. ‡P<0.05 versus hSlit2 1 µg-treated IRI mice. §P<0.05 versus N-mSlit2–treated IRI mice.

The change in renal function was associated with parallel changes in morphology (Figure 5, A–D). After IRI, there was a marked increase in tubular injury compared with sham mice (Figure 5, A, B, and E, P<0.05). Both hSlit2 and N-mSlit2 administration reduced this injury (Figure 5, C and E, P<0.05 N-mSlit2 versus vehicle, and Supplemental Figure 7, P<0.05 hSlit2 versus vehicle). In contrast, blockade of N-mSlit2 with RoboN before administration to IRI mice attenuated the tubuloprotective effects of Slit2 (Figure 5, D and E, P<0.05).

Figure 5.
Figure 5.

Slit2 improves acute tubular necrosis and reduces neutrophil infiltration after renal IRI. (A–D) Representative hematoxylin and eosin-stained kidney sections from mice subjected to (A) sham surgery, (B) vehicle administration before IRI, (C) N-mSlit2 administration before IRI, and (D) N-mSlit2–RoboN administration before IRI examined using a Zeiss AxioSkop microscope equipped with a SPOT-RT Camera. Original magnification, ×20; ×2 in insets. (E) To quantify the degree of tubular injury, kidney sections were examined using a Zeiss AxioSkop microscope and scored by counting the percentage of tubules that displayed cell necrosis, loss of brush border, cast formation, and tubular dilation; they were scored as follows: 1<10%, 2=10%–25%, 3=26%–50%, 4=51%–75%, and 5>75%. Two to three fields from the outer medulla of each section were evaluated. Original magnification, ×200. (F) Experiments were performed as in Figure 4, and kidneys were collected after 18 hours. Kidneys were weighed, minced, and digested with collagenase type IA (10 µg/ml). The cell pellet was washed, nonspecific Fc binding was blocked with anti-mouse CD16/32 antibody (2.4G2), and cell suspensions were incubated with fluorophore-tagged anti-mouse CD45 antibody (30-F11) to determine total leukocyte cell numbers. Anti-CD45 antibody-labeled samples were further labeled with anti-mouse GR-1-FITC antibody (Ly6G) and anti-mouse CD11b-PE antibody to identify neutrophils. Appropriate fluorochrome-conjugated, isotype-matched, irrelevant monoclonal antibodies were used as negative controls. Flow cytometry data acquisition was performed on BD FACS Calibur, and data were analyzed using FlowJo software 6.4. The number of GR-1+CD11b+CD45+ neutrophils was normalized to kidney weight, indexed to the value for sham surgery kidneys, and log-transformed to generate a neutrophil infiltration score. Mean values ± SEM from experiments involving four to seven mice per experimental group. ATN, acute tubular necrosis. *P<0.05 versus sham-operated mice. †P<0.05 versus vehicle-treated IRI mice. ‡P<0.05 versus N-mSlit2–treated IRI mice.

IRI also led to an increase in renal neutrophil infiltration compared with sham-operated controls (Figure 5F, P<0.05). N-mSlit2 treatment reduced renal neutrophil numbers (P<0.05 versus vehicle), whereas preincubation of N-mSlit2 with RoboN abrogated this effect (Figure 5F, P<0.05). Preadministration of hSlit2 also reduced renal neutrophil and macrophage infiltration (Supplemental Figure 8, P<0.05 versus vehicle). Collectively, these data show that Slit2 administration reduces IRI-induced renal dysfunction, structural injury, and neutrophil infiltration into the injured kidney.

Slit2 Does Not Inhibit Neutrophil Phagocytosis, Superoxide Production, or Bacterial Killing In Vitro

Because renal IRI is often associated with critical illness, where infection is a common occurrence, we questioned whether exogenous Slit2 might inhibit protective neutrophil immune functions, such as phagocytosis of opsonized particles and superoxide production.35 Using a latex bead phagocytosis assay, we found that Slit2 did not affect neutrophil phagocytosis, with 77.7%±7.1% of untreated neutrophils and 80.6%±7.0% of Slit2-treated neutrophils ingesting at least one opsonized bead (untreated versus Slit2-treated mean phagocytic index: 3.5±0.6 versus 3.7±0.4).

Using an assay of superoxide production, we next tested whether Slit2 inhibits the respiratory burst after neutrophil activation.22 Although unstimulated neutrophils did not produce detectable superoxide (data not shown), formyl-methionyl-leucyl-phenylalanine (fMLP) treatment enhanced neutrophil superoxide production to 20.6±0.6 nmol/107 cells per minute. Preincubation of neutrophils with Slit2 did not impair superoxide production but rather, promoted a modest increase (27.8±1.2 nmol/107 cells per minute, P<0.05).

We next tested the effects of Slit2 on neutrophil killing of the extracellular pathogen Staphylococcus aureus, a common cause of bacterial sepsis in critically ill patients with renal IRI. After bacteria were incubated with neutrophils for 90 minutes, the bacterial colony count in the untreated neutrophil sample decreased to 61%±13% of the starting count, whereas the bacterial count in the Slit2-treated neutrophil samples displayed an even greater reduction (Figure 6A, P<0.05). Thus, Slit2 did not impair neutrophil killing of S. aureus but rather, enhanced it.

Figure 6.
Figure 6.

Slit2 does not inhibit neutrophil killing of the extracellular pathogen S. aureus or increase hepatic bacterial load after infection with the intracellular pathogen L. monocytogenes. (A) Human neutrophils (1.5×106) were incubated with N-mSlit2 or control vehicle at 37°C for 10 minutes, and then, 10% human serum and S. aureus (methicillin-resistant S. aureus strain CMRSA-10/USA300 at 1×106 CFU) were added. Samples were incubated at 37°C with 200 rpm shaking for 90 minutes. The number of viable bacteria in these suspensions was determined by plating. (B) N-mSlit2 or control vehicle was administered intravenously by tail vein injection, and L. monocytogenes (5×104 CFU in 200 µl PBS) was injected intravenously 1 hour later. At the indicated time points, mice were euthanized, the left lobe of liver was homogenized in sterile PBS, and bacterial load was determined from serial dilutions on brain heart infusion-agar plates. Mean values ± SEM from six mice per experimental group. *P<0.05 versus input control. †P<0.05 versus polymorphonuclear leukocytes alone.

Slit2 Treatment Does Not Impair Immune Protection against Bacterial Infection In Vivo

To further explore the effect of Slit2 on innate immunity, we tested its actions in two established models of infection. First, Slit2 was administered to mice inoculated with the intracellular pathogen Listeria monocytogenes. At all times ranging from 0.5 to 48 hours, hepatic bacterial counts, reflective of neutrophil activity, were similar between vehicle- and Slit2-treated mice (Figure 6B), indicating that Slit2 administration does not impair protective innate immune responses against intracellular pathogens.36

We also tested the effects of administering Slit2 on clearance of uropathogenic Escherichia coli in a murine model of ascending urinary tract infection.37,38 Because neutrophils are essential for antibacterial defense of the genitourinary tract, we assessed the effects of Slit2 on neutrophil recruitment and bacterial clearance.39,40 Neutrophil numbers in the urine and bacterial colony counts in the urine and kidney were similar between vehicle- and Slit2-treated mice (Figure 7). Taken together, these results suggest that Slit2 administration does not impair immune protection against bacterial infections in vivo.

Figure 7.
Figure 7.

Slit2 does not impair neutrophil recruitment or bacterial clearance in a model of E. coli ascending urinary tract infection. N-mSlit2 (2 µg) or control vehicle was injected intravenously into mice 1 hour before intravesical inoculation with 109 CFU/ml (100 µl) uropathogenic E. coli CFT073 suspension; 6 and 24 hours later, urine was collected in a sterile fashion, and mice were euthanized. The kidneys were collected aseptically and homogenized, and 0.1 ml each homogenate were plated on tryptic soya agar. The number of colonies was scored after overnight culture at 37°C. (A) Urinary neutrophil concentration was calculated by hemocytometer analysis of fresh urine samples. Bacterial colony counts from (B) urine and (C) kidney homogenates are presented as log CFU per milliliter. Results were obtained from n=6 mice per group.

Discussion

AKI continues to exact high rates of morbidity and mortality in hospitalized patients,41 with IRI being the leading cause of AKI in both native and transplanted kidneys.42,43 After IRI, the injured kidney synthesizes proinflammatory cytokines and chemokines, most notably TNF-α and IL-8, that promote renal neutrophil infiltration, a process important for IRI pathogenesis.11,44,45 Therapies that block a specific aspect of neutrophil recruitment, such as neutrophil–endothelial adhesion, are only partially protective in mouse models of AKI.13,14,46,47 We report that Slit2 may represent a potent strategy to inhibit multiple steps in the pathologic neutrophil recruitment seen in AKI, thus attenuating renal injury and dysfunction.

The Slit family of secreted glycoproteins was originally described in Drosophila as a group of neuronal repellents during central nervous system development.16,17,48 We and others have previously shown that the Slit2 receptor, Robo-1, is also detected on leukocyte subsets, including neutrophils, T lymphocytes, monocytes, and dendritic cells.21–23 Similar to its effects on directional axonal growth, Slit2 also inhibits leukocyte chemotactic migration.20–22

Here, we show that Slit2 affects not only chemotaxis of neutrophils but also, other key steps in neutrophil recruitment, such as capture, adhesion, and transendothelial migration. All of these processes, including initial neutrophil capture, involve actin cytoskeletal rearrangements, which in turn, are regulated by Rho-family GTPases, including RhoA, Cdc42, and Rac.32,49–58 Through binding to Robo receptors, Slit2 can regulate the activity of Rho-family GTPases. Indeed, we previously showed that, in neutrophils, Slit2 signals through Robo-1 to inhibit chemoattractant-induced polarization and activation of Rac2 and Cdc42.22 Similarly, Slit2 inhibited chemoattractant-induced Rac activation and chemotaxis in Jurkat T cells.21 Our work is, thus, in keeping with the work of others showing that inhibition of Cdc42 or loss of Rac activity impairs leukocyte migration across the endothelial barrier.32,54–56 More broadly, these data suggest that Slit2 may act as a master negative switch of leukocyte recruitment processes through inhibition of Rho-family GTPases.

We hypothesized that systemic Slit2 administration would attenuate kidney IRI through binding to Robo-1 on circulating neutrophils, rendering them less responsive to local recruitment signals from the IRI kidney. Using a murine model of renal IRI, we showed that Slit2 administration significantly attenuated the rise in plasma creatinine, tubular injury, and renal neutrophil infiltration observed in mice after IRI. Similar to our findings, prior studies showed that Slit2 administration can ameliorate renal inflammation associated with crescentic GN59 and suppress contact hypersensitivity responses.20 Collectively, these observations show the potent anti-inflammatory properties of Slit2 in certain settings and suggest its potential as a novel therapy to prevent inflammation of diverse etiologies.

Although neutrophils are an important contributor to renal IRI pathogenesis, they also play a critical role in maintaining protective immunity against pathogens. In this regard, we found that, although Slit2 impairs chemoattractant-induced neutrophil migration,22 it does not have a deleterious effect on protective innate immune neutrophil functions, such as phagocytosis or superoxide production. Our findings are in accordance with a previous study showing that Slit2 does not impair superoxide production by HL-60 neutrophil-like cells.23 The varying effects of Slit2 on different neutrophil functions may be potentially explained by the complex and not fully understood roles that Rho-family GTPases play in the regulation of these processes.60–63 Indeed, although polarization and activation of Rac and Cdc42 are known to control directional neutrophil migration,64 their involvement in the regulation of phagocytosis is more complex. Whereas Rac1-deficient neutrophils show intact Fc (fragment, crystallizable)-mediated phagocytosis and NADPH oxidase activity, Rac2-deficient neutrophils display markedly diminished NADPH oxidase activity and phagocytosis.60–62 In contrast, loss of Cdc42 results in normal phagocytosis and increased superoxide production.63 In line with this report, we found that Slit2 enhanced killing of S. aureus, and Slit2 treatment of L. monocytogenes-infected mice did not increase hepatic bacterial load; both of these processes are superoxide-dependent.65–68 In this context, our results suggest that Slit2 may selectively target polarization-dependent amplification responses within neutrophils, although the precise mechanisms through which this process may occur remain to be elucidated.

Recruitment of neutrophils to sites of injury is a complex process tightly regulated by a balance of attractant and repellent signals. After IRI, we showed that, coincident with a large neutrophil influx, endogenous levels of Slit2 in the mouse kidney are significantly reduced. Furthermore, systemic administration of exogenous Slit2 blocked neutrophil recruitment to the IRI kidney. In contrast, Slit2 treatment of mice with an E. coli-ascending urinary tract infection did not affect neutrophil recruitment or clearance of bacteria from the urine or kidney. These results point to the context-specific effects of Slit2 on neutrophil recruitment. Indeed, because IRI and bacterial infection can activate different sets and magnitudes of attractant and/or repellent signals, it is possible that the Slit2 responsiveness of neutrophils might vary depending on the specific balance of signals that they receive. Although beyond the scope of this study, the precise determinants of the neutrophil response to Slit2 deserve additional exploration. Nevertheless, our observation that Slit2 does not impair neutrophil antibacterial defenses points to its potential clinical use to prevent IRI without causing unwanted immunosuppression.

Neutrophils are an important mediator of renal IRI, but other cells, including macrophages, dendritic cells, and platelets, also contribute to IRI pathogenesis.8,11 Thus, although Slit2 inhibits neutrophil recruitment in renal IRI, it may also act on other cell subsets implicated in AKI. We recently showed that Slit2 is a potent antiplatelet agent in vitro and in vivo.69 Because activated platelets cause microvascular thrombosis in IRI, it is possible that Slit2 administration attenuated renal injury, in part, through its antiplatelet effects.70–74 However, because platelet inhibition only partially ameliorates AKI,75 the antiplatelet effects of Slit2 do not fully explain our results. Similarly, although Slit2 administration also reduced macrophage infiltration into the IRI kidney (Supplemental Figure 8B), agents targeting macrophages alone only partially attenuate renal injury.76 Thus, despite the dominant role of neutrophils in the pathogenesis of renal IRI, the antineutrophil effects of Slit2 may be only one of several renoprotective activities of this pleiotropic molecule.44,45,77

AKI resulting from IRI remains a complex and challenging clinical problem. We report that Slit2 reduces neutrophil capture, adhesion, and transendothelial migration in vitro and prevents neutrophil infiltration, tubular injury, and renal failure after IRI in vivo. We also show that Slit2 does not impair protective neutrophil immune functions or enhance susceptibility to bacterial infection. These properties position Slit2 as an ideal therapeutic candidate for the prevention and treatment of renal IRI.

Concise Methods

Chemicals and Reagents

Unless otherwise stated, reagents were purchased from Sigma-Aldrich (St. Louis, MO). Polymorphprep neutrophil separation medium was from Axis-Shield (Norway). Transwell inserts were from Corning Costar. Except as noted, all antibodies were from eBioscience (San Diego, CA) and used at a concentration of 5 µg/ml.

Slit2 Expression and Purification

Production of full-length hSlit2 and myc antibody-affinity purification were performed as previously described.22 Bioactive truncated N-mSlit2 and N-hSlit2 were purchased from R&D systems (Minneapolis, MN) and Peprotech (Rocky Hill, NJ), respectively.

Isolation of Primary Human Neutrophils

Human whole blood was obtained from healthy volunteers, and neutrophils were isolated using Polymorphprep gradient separation as previously described.22 Before use, neutrophils were resuspended in HBSS containing 1 mM CaCl2 and 1 mM MgCl2. Experiments were performed within 1–2 hours of isolating neutrophils.22

Immunofluorescent Labeling of Neutrophils

Human neutrophils were seeded on fibronectin-coated coverslips and immunofluorescently labeled as previously described.22 Cells were fixed in 4% paraformaldehyde, permeabilized, and incubated with rabbit anti-human Robo-1 antibody followed by Alexa 594-conjugated anti-rabbit IgG together with 4',6-diamidino-2-phenylindole. Cells were visualized with a spinning disc DMIRE2 confocal microscope (Leica Microsystems, Toronto, Canada) equipped with a Hamamatsu back-thinned electron microscopy charge-coupled device camera.22

Neutrophil–Endothelial Adhesion Assays

Neutrophil–endothelial adhesion assays were performed with minor modifications as previously described.78–80 Freshly isolated human neutrophils were labeled with calcein and incubated with medium alone or Slit2 (4.5 µg/ml) for 10 minutes.22 In some experiments, Slit2 was premixed with molar equivalent amounts of RoboN for 10 minutes at 37°C before incubating with neutrophils. Neutrophils (105 cells/well) were incubated with confluent HUVEC monolayers and allowed to adhere for 30 minutes.81 Nonadherent cells were removed by centrifuging the 96-well plates upside down at 100 × g for 1 minute. Neutrophil adhesion was quantified using a fluorescent plate reader at excitation and emission wavelengths of 494 and 517 nm, respectively. In some wells, HUVEC were incubated with TNF-α for 4 hours before incubating with neutrophils. In parallel experiments, either neutrophils or HUVEC were incubated with Slit2 for 10 minutes, and unbound Slit2 was removed by washing before performing neutrophil–endothelial cell adhesion assays.

H/R of Endothelial Cells

To simulate IRI in an in vitro system, HUVEC were grown in endothelial basal medium-2 and maintained at 37°C in a standard incubator at room air oxygen tension (21% oxygen). Hypoxic conditions were induced by exposing cells to 1% oxygen and balance nitrogen at 37°C.82 Ambient PO2 within the chamber was calibrated and monitored during the entire experiment using a Proox 110 oxygen controller system (Biospherix). Cells were exposed to 2 hours of hypoxia followed by variable periods of reoxygenation ranging from 0.5 to 3 hours using previously described protocols.83–86 In some wells, HUVEC were incubated with TNF-α.87

RT-PCR

Total RNA was isolated from HUVEC using one-step RNA reagent (BIO BASIC INC, Unionville, Canada) following the manufacturer’s instructions. RT-PCR was performed using QIAGEN One-Step RT-PCR Kit (QIAGEN, Toronto, Canada) with 1 µg total RNA. The primers for human Robo-1 to -4 and corresponding RT-PCR product sizes are provided in Supplemental Table 1. Reaction mixtures were subjected to the amplification procedure as per the manufacturer’s instructions. PCR products were separated by 1.5% agarose gel electrophoresis.

3-(4, 5-Dimethylthiazol-2-yl)-2,5-Diphenyltetrazolium Bromide Assays

To determine the viability of cells after H/R injury, 3-(4, 5-dimethylthiazol-2-yl)-2,5-diphenyltetrazolium bromide assays were performed as per the manufacturer’s instructions.30 Mitochondrial dehydrogenases of viable cells cleave the tetrazolium ring, yielding purple formazan crystals that are insoluble in aqueous solutions. Crystals were dissolved in acidified isopropanol, and results were read spectrophotometrically at a wavelength of 570 nm. The background absorbance was measured at 670 nm and subtracted from the 570-nm measurement. In some experiments, cells were exposed to staurosporin (1 µM) for 2 hours. All experiments were carried out in triplicate.

Microfluidic Neutrophil Adhesion Assays

To study neutrophil–endothelial interactions under shear flow, we used a microfluidics system as previously described.69,88–93 HUVECs were grown to confluence in channels of the Bioflux microfluidic system (Fluxion Biosciences, CA) coated with fibronectin (50 µg/ml) and incubated with TNF-α for 4 hours at 37°C. Calcein-labeled human neutrophils (3×105/well) were preincubated with Slit2 (4.5 µg/ml) for 10 minutes and then perfused through the channels at a shear rate of 0.5 dynes/cm2.94,95 In some experiments, Slit2 (4.5 µg/ml) was premixed with molar equivalent amounts of RoboN for 10 minutes at 37°C before incubating with neutrophils. The plates were placed on the heated stage of a Nikon TE2000 inverted microscope and visualized using a 20× objective. Sequential images were recorded every 6 seconds for up to 12 minutes in a representative field using Volocity software (Perkin-Elmer, Woodbridge, ON, Canada) interfaced with a Hamamatsu video camera. At the end of this period, four additional fields were each recorded for 30 seconds. Neutrophil adhesion was quantified with Bioflux Montage software (Fluxion Biosciences). In other experiments, neutrophil–endothelial interactions were recorded at 1 minute after initiation of flow, and the number of rolling and arrested neutrophils was determined. Only cells that remained stationary for at least 6 seconds were defined as stably adherent.96

Neutrophil Transendothelial Migration Assays

Neutrophil transendothelial migration assays were performed as previously described.97,98 HUVEC were grown to confluence on fibronectin-coated polyester transwell inserts (diameter=6.5 mm, pore size=3 μm; Corning Costar) placed in a 24-well plate. Human neutrophils (5×106 cells/ml) were labeled with calcein and then incubated with Slit2 (4.5 µg/ml) for 10 minutes at 37°C. Thereafter, neutrophils (5×105/well) were placed in the upper well of the transwell chamber, and the chemokine IL-8 (50 ng/ml) was added to the lower well.33 Neutrophils were allowed to migrate for 3 hours at 37°C. At the end of 3 hours, the neutrophils that had migrated from the upper to the lower well were permeabilized with 1% Triton, and the resulting lysates were transferred in triplicate to a 96-well plate. The fluorescence emitted was read using a fluorescent plate reader at excitation and emission wavelengths of 494 nm and 517 nm, respectively.33 In some experiments, HUVEC were exposed to H/R as described above.

Neutrophil Phagocytosis Assays

Neutrophil phagocytosis of opsonized particles was assessed as previously described.99 Briefly, 3.8-µm latex beads (Bang Laboratories, Inc., IN) were coated with human IgG (1 mg/ml) for 2 hours at room temperature. Neutrophils were preincubated with anti-myc Ab affinity-purified Slit2 (0.6 µg/ml) or control medium for 10 minutes, and then, they were exposed to opsonized latex beads, rapidly centrifuged (1000 rpm for 30 seconds) to initiate phagocytosis, and plated onto fibronectin-coated coverslips. Phagocytosis was terminated after 30 minutes, and external beads were labeled on ice using Cy2-conjugated anti-human IgG. Images were recorded for at least 10 random fields using a Leica deconvolution microscope (40× objective). The number of ingested particles was analyzed by counting total beads using differential interference contrast microscopy and subtracting the number of external labeled beads. Two measures were used to assess phagocytosis: (1) percent of neutrophils with at least one ingested bead and (2) phagocytic index (number of ingested beads per number of cells).99

Neutrophil Superoxide Production Assays

Superoxide production was assayed by measuring the superoxide dismutase inhibitable reduction of cytochrome c.99 Briefly, neutrophils (2.5×105 cells) were incubated with anti-myc Ab affinity-purified Slit2 (0.6 µg/ml) or control medium, suspended in PBS supplemented with divalent cations and glucose, and incubated with cytochrome c (75 μM) ± superoxide dismutase (60 μg/ml). Neutrophils were then stimulated with fMLP (1 μM), and cytochrome c reduction was assayed by measuring absorbance at 550 nm using a VersaMax Microplate Reader (Molecular Devices, Sunnyvale, CA) in kinetic mode for 20 minutes and acquiring readings every 15 seconds.

Neutrophil Killing of S. aureus

Human neutrophils (1.5×106) were incubated with N-mSlit2 or vehicle control at 37°C for 10 minutes, and then, 10% human serum and S. aureus (methicillin-resistant S. aureus strain CMRSA-10/USA300; 1×106 CFU; a gift from Andrew Simor, Sunnybrook Health Sciences Centre, Toronto, Canada) was added.66 Samples were incubated at 37°C with 200 rpm shaking for 90 minutes. The number of viable bacteria in these suspensions was determined by plating.66

Mouse Renal IRI

Kidney ischemia–reperfusion surgery was performed using male C57BL/6 mice (8–12 weeks of age; Charles River Laboratories, Wilmington, MA) as previously reported.26,45 The core temperature of the mice was maintained between 34°C and 36°C with a heating pad, and bilateral flank incisions were made under anesthesia (ketamine, 12 mg/ml; atropine, 0.48 mg/ml; xylazine, 24 mg/ml; 200 µl mixture administered per 20 g body weight). Both renal pedicles were exposed and cross-clamped for 26 minutes. Clamps were removed, and kidneys were allowed to reperfuse for 18 hours before analysis. Ambient postoperative air temperature was maintained between 30°C and 32°C until mice had fully recovered. Sham-treated mice were subjected to similar surgery without clamping of the renal pedicles. Mice were injected intraperitoneally with full-length hSlit2 at the indicated doses, N-mSlit2 (2 µg), N-mSlit2 (2 µg) premixed with molar equivalent amounts of RoboN, or vehicle control 1 hour before induction of IRI. After 18 hours, mice were euthanized, and kidneys were harvested. Before euthanasia, blood was drawn by retro-orbital bleed, and plasma creatinine was determined using a colorimetric assay according to the manufacturer's protocol (Sigma Aldrich).25,26 All animal experiments were approved by the University of Virginia and Hospital for Sick Children Institutional Animal Care and Use Committees, and they adhered to the National Institutes of Health Guide for the Care and Use of Laboratory Animals.

Histologic Scores

Kidney sections (4 μm) were stained with hematoxylin and eosin, and images were obtained using a SPOT-RT Camera (software version 3.3; Diagnostic Instruments, Sterling Heights, MI) under 2× and 20× magnifications. For quantification of tubular injury score, sections were assessed by counting the percentage of tubules that displayed cell necrosis, loss of brush border, cast formation, and tubule dilation as follows: 1<10%, 2=10%–25%, 3=26%–50%;, 4=51%–75%, and 5>75%. Two to three fields from each outer medulla were evaluated and scored separately by two individuals masked to treatment categories.26

Flow Cytometry Analysis

After IRI, flow cytometry was used to quantify the infiltrating leukocyte subsets in the injured kidney.25 In brief, kidneys were harvested, weighed, minced, and incubated with collagenase type IA (10 µg/ml; Sigma-Aldrich) in cold Dulbecco’s PBS buffer with EDTA (2 mmol/L) for 15 minutes at 37°C. The digested kidney tissue suspension was teased through a 100-µm BD Falcon cell strainer (Fisher Scientific, Pittsburgh, PA) by the rubber end of a 1-ml syringe plunger, passed through a cotton column treated with 10% FCS, and centrifuged at 1200 rpm for 10 minutes. The cell pellet was washed with 1% BSA in PBS containing 0.1% sodium azide (Sigma-Aldrich). After blocking nonspecific Fc binding with anti-mouse CD16/32 antibody (2.4G2), fresh cell suspensions were incubated with fluorophore-tagged anti-mouse CD45 antibody (30-F11) to determine total leukocyte cell numbers. Anti-CD45 antibody-labeled samples were also labeled with different combinations of anti-mouse F4/80-APC antibody (BM8), anti-mouse GR-1-FITC antibody (Ly6G), and anti-mouse CD11b-PE antibody to identify macrophages (CD11b+ F4/80low) and neutrophils (CD11b+ GR1+).25 7-AAD (BD Biosciences, San Jose, CA) was added 15 minutes before analyzing the sample to separate live from dead cells.25 Appropriate fluorochrome-conjugated, isotype-matched, irrelevant monoclonal antibodies were used as negative controls. Subsequent flow cytometry data acquisition was performed on BD FACS Calibur. Data were analyzed using FlowJo software 6.4 (Tree Star).25 The number of GR-1+CD11b+CD45+ neutrophils was normalized to kidney weight, indexed to the value for sham surgery kidneys, and log-transformed to generate a neutrophil infiltration score. Similarly, the number of CD11b+ F4/80low macrophages was normalized to kidney weight and indexed to the value of sham surgery kidneys to generate a macrophage infiltration score.

Slit2 Immunofluorescent Labeling

Immunofluorescent staining was performed on frozen sections of mouse kidney. Microwave antigen retrieval was carried out in citrate buffer for 20 minutes at medium-high setting (950 W maximum output, Panasonic NN-S758WC; Panasonic, Mississauga, ON, Canada) followed by 30 minutes of cooling at room temperature.100 Sections were blocked and permeabilized in 2% donkey serum with 1% BSA and 0.1% Triton-X for 45 minutes and then incubated with anti-Slit2 antibody (8 µg/ml; Santa Cruz Biotech) at 4°C overnight. An Alexa 488-conjugated secondary antibody (1.5 µg/ml) in blocking reagent was incubated at room temperature for 2 hours. For some slides, autofluorescence of the surrounding renal cortex was captured in the red channel. For quantification, slides were treated with 0.05% sudan black (Sigma-Aldrich, St. Louis, MO) in 70% ethanol for 30 minutes at room temperature to reduce renal autofluorescence.101 Kidney sections were mounted and visualized using a spinning disk DMIRE2 confocal microscope (Leica Microsystems, Toronto, ON, Canada) equipped with a Hamamatsu backthinned electron microscopy charge-coupled device camera. Images were acquired at 20× magnification and analyzed using Volocity software (Perkin-Elmer, Woodbridge, ON, Canada).

Murine Infection with Listeria Monocytogenes

Six- to eight-week-old C57BL/6J mice were purchased from Jackson Laboratory. N-mSlit2 (2 µg/mouse) or control vehicle was delivered by intravenous injection in the lateral tail vein. L. monocytogenes (5×104 CFU) in 200 µl PBS was injected intravenously 1 hour later. Mice were euthanized at the indicated time points, and the livers were harvested. The left lobe of the liver was homogenized in sterile PBS for quantification of bacterial CFU from serial dilutions on brain heart infusion-agar plates. These experiments were approved by the Hospital for Sick Children Institutional Animal Care and Use Committee and adhered to the National Institutes of Health Guide for the Care and Use of Laboratory Animals.

Experimental Acute Pyelonephritis

As previously described, E. coli CFT073 was isolated from the blood and urine of a patient with acute pyelonephritis.102 The functional virulence genes in E. coli CFT073 include hly1+, pap1+, sfa1+, and pil1+ as well as TcpC. In vivo, this strain is highly virulent in a mouse model of ascending urinary tract infection and exhibits in vitro cytotoxicity in cultured human renal proximal tubular epithelial cells.103 The strains were grown at 37°C on solid Luria–Bertani agar and suspended in 10 ml PBS (pH 7.2) to generate the bacterial suspension used for infection (109 CFU/ml).

The ascending murine urinary tract infection experiments were performed as previously described.37–39 Briefly, after isoflurane anesthesia, male BALB/c mice (8–12 weeks) were infected by intravesical inoculation (109 CFU/ml, 100 µl) through a soft polyethylene catheter (outer diameter=0.61 mm; Clay Adams, Parsippany, NY). The catheter was withdrawn, and the mice were allowed food and water ad libitum. One hour before inoculation, mice were intraperitoneally administered either N-mSlit2 (2 µg) or PBS vehicle. After designated time intervals, urine was collected into sterile tubes through gentle suprapubic pressure. After euthanasia, kidneys were retrieved using aseptic technique.

Bacterial numbers in urine and kidney homogenates were determined by viable counts. The organs were separately placed in a sterile plastic bag containing 5 ml PBS and homogenized in a Stomacher 80 homogenizer (Seward Medical, UAC House, London, United Kingdom). Homogenates were diluted in sterile PBS, and 0.1 ml each dilution were plated on tryptic soya agar. The number of colonies was scored after overnight culture at 37°C. Urine neutrophils were quantified on freshly isolated urine samples in a hemocytometer chamber as previously described.38,39 The study was approved by the Animal Experiment Ethics Committee at the Lund district court in Sweden.

Statistical Analyses

All data are shown as mean ± SEM unless otherwise stated. Graphpad Prism (version 5.0; GraphPad Software, San Diego, CA) and SPSS statistical software (version 19.0; SPSS, Chicago, IL) were used to analyze the data. Data were analyzed using two-tailed t test or one-way ANOVA with posthoc analysis as appropriate. P<0.05 was used to indicate significance.

Disclosures

None.

Acknowledgments

The authors thank Dr. James Scholey (University of Toronto) for helpful discussions.

D.A.Y. was supported by a Canadian Society of Transplantation Fellowship and a Canadian Institutes of Health Research Fellowship. This work was supported in part by National Institutes of Health Grants R01DK062324 (to M.D.O.) and R01DK085259 (to M.D.O.), Canadian Institutes of Health Research Grant MOP-111083 (to L.A.R.), and a Kidney Foundation of Canada grant (to L.A.R.). L.A.R. holds a Canada Research Chair (Tier 2) and was also supported by an Early Researcher Award from the Ministry of Research and Innovation.

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Slit2 Prevents Neutrophil Recruitment and Renal Ischemia-Reperfusion Injury
Swasti Chaturvedi, Darren A. Yuen, Amandeep Bajwa, Yi-Wei Huang, Christiane Sokollik, Liping Huang, Grace Y. Lam, Soumitra Tole, Guang-Ying Liu, Jerry Pan, Lauren Chan, Yaro Sokolskyy, Manoj Puthia, Gabriela Godaly, Rohan John, Changsen Wang, Warren L. Lee, John H. Brumell, Mark D. Okusa, Lisa A. Robinson
JASN Aug 2013, 24 (8) 1274-1287; DOI: 10.1681/ASN.2012090890
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