- Research article
- Open Access
Perforin enhances the granulysin-induced lysis of Listeria innocua in human dendritic cells
© Walch et al; licensee BioMed Central Ltd. 2007
- Received: 08 June 2007
- Accepted: 16 August 2007
- Published: 16 August 2007
Cytotoxic T lymphocytes (CTL) and natural killer (NK) cells play an essential role in the host defence against intracellular pathogens such as Listeria, and Mycobacteria. The key mediator of bacteria-directed cytotoxicity is granulysin, a 9 kDa protein stored in cytolytic granules together with perforin and granzymes. Granulysin binds to cell membranes and is subsequently taken up via a lipid raft-associated mechanism. In dendritic cells (DC) granulysin is further transferred via early endosomes to L. innocua-containing phagosomes were bacteriolysis is induced. In the present study we analysed the role of perforin in granulysin-induced intracellular bacteriolysis in DC.
We found granulysin-induced lysis of intracellular Listeria significantly increased when perforin was simultaneously present. In pulse-chase experiments enhanced bacteriolysis was observed when perforin was added up to 25 minutes after loading the cells with granulysin demonstrating no ultimate need for simultaneous uptake of granulysin and perforin. The perforin concentration sufficient to enhance granulysin-induced intracellular bacteriolysis did not cause permanent membrane pores in Listeria-challenged DC as shown by dye exclusion test and LDH release. This was in contrast to non challenged DC that were more susceptible to perforin lysis. For Listeria-challenged DC, there was clear evidence for an Ca2+ influx in response to sublytic perforin demonstrating a short-lived change in the plasma membrane permeability. Perforin treatment did not affect granulysin binding, initial uptake or intracellular trafficking to early endosomes. However, enhanced colocalization of granulysin with listerial DNA in presence of perforin was found by confocal laser scanning microscopy.
The results provide evidence that perforin increases granulysin-mediated killing of intracellular Listeria by enhanced phagosome-endosome fusion triggered by a transient Ca2+ flux.
- Dendritic Cell
- Hemolytic Activity
- Early Endosome
CTL and NK cells play an essential role in the host defence against intracellular microbial pathogens like Listeria monocytogenes  or Mycobacteria tuberculosis . Several mechanisms are involved in clearance of intracellular bacteria including cytokine release , apoptosis induction of the host cell , and directly executed antimicrobial activity of CTL. The direct antibacterial activity of CTL is mediated by granulysin , a 9 kDa protein discovered by subtractive hybridization of late activated T-cells [6, 7]. Recombinant granulysin proved to exhibit a broad spectrum of antimicrobial activity against bacteria, fungi and parasites . We recently demonstrated that granulysin enters human DC in a lipid raft-associated mechanism and gains access to L. innocua located in phagosomes to induce bacteriolysis . However, intracellular bacteria were never fully eradicated by treatment of the DC with granulysin only. As granulysin is stored in granules of CTL together with other lytic proteins such as perforin, the interaction of both proteins in killing intracellular bacteria is of great interest. Perforin shares homology with the terminal complement components and can thus multimerize in eukaryotic membranes to form pores of a diameter of 50 nm or less. These perforin pores were initially thought to allow passage of lytic granule components, especially granzymes, to the target cell cytosol [10–13]. The discovery of granzyme B to be endocytosed independently of perforin as well as the induction of target cell apoptosis by granzyme B and perforin without detectable leakage of the plasma membrane questioned the pore formation model [14, 15]. In contrary, Keefe et al. demonstrated a transient Ca2+ flux in HeLa cells in response to sublytic perforin concentrations indicating short-lived membrane pores that are immediately repaired by the cellular wound healing system .
The role of perforin in granulysin-mediated intracellular bacteriolysis is contradictory. Stenger et al. demonstrated that perforin was necessary for granulysin-mediated killing of intracellular M. tuberculosis in macrophages . On the other hand, cell based in vitro-studies showed that killing of intracellular Mycobacteria by CD4+ and CD8+ cytotoxic T cells occurred independently of perforin . The role of perforin in delivering granulysin was further questioned in a study using M. leprae also residing within phagosomes of host cells. Ochoa et al. demonstrated by phenotyping cells in dermal granuloma of leprosy lesions that the majority of cells containing granulysin were CD4+ and CD3+, but negative for perforin .
Using our proven model system, we investigated the interaction of perforin and granulysin in human monocyte-derived DC as hosts harbouring L. innocua, a gram positive, apathogenic bacterium ubiquitously distributed in our environment . Influence of perforin on granulysin binding, uptake and trafficking was visualized and quantified as well as correlated to the lysis of intracellular L. innocua. It was further examined if stable plasma membrane pore formation and/or short lived changes in the plasma membrane integrity allowing transient Ca2+ fluxes is a prerequisite for the mediation of the perforin effect.
Perforin enhances significantly granulysin-mediated lysis of L. innocua in DC
In order to exclude bacterial loss due to detachment of perishing host cells, the viability of Listeria-challenged DC during incubation with granulysin alone or in combination with perforin was assessed in LDH release assays. Granulysin in all tested concentrations did not cause a significant LDH release from DC (Fig. 1b). Incubation of granulysin (2.5 μM) with perforin (2.5 kU/ml) resulted in DC lysis of less than 2% (Fig. 1b). Therefore, 2.5 μM granulysin and 2.5 kU/ml perforin were considered to be sublytic to host cells and were used in all subsequent experiments. Perforin incubated alone in concentrations up to 10 kU/ml was found to have no lytic activity on Listeria-challenged DC (LDH release < 7%). This result further indicates that perforin in the concentrations applied does not lead to an increase in membrane permeability sufficient for a detectable release of LDH from treated DC.
L. innocua in suspension treated with granulysin showed dose-dependently a decrease in viability as calculated from bacterial growth curves. At granulysin concentrations down to 1.5 μM more than 90% of the bacteria were killed (Fig. 1c). The median effective dose was determined in the concentration range of 0.4 to 0.8 μM. Below 0.2 μM killing activity decreased to background level. Unlike to the killing efficiency of intracellular L. innocua, simultaneous perforin application at a concentration of 2.5 kU/ml did not further decrease bacteriaviability in suspension. Furthermore, perforin applied alone in concentrations up to 10 kU/ml did not affect Listeria viability (data not shown).
Taken together, granulysin-mediated lysis of intracellular L. innocua in human DC is significantly enhanced by perforin.
Granulysin and perforin can be sequentially added to induce enhanced intracellular bacteriolysis
Sublytic perforin does not result in stable plasma membrane pores
Stable perforin membrane pores could be excluded to be a major factor for the enhancement effect in granulysin-mediated bacteriolysis.
Sublytic perforin induces a transient Ca2+ influx
To investigate the source of the Ca2+ responsible for the transient flux, Listeria-challenged DC were pretreated with the established intracellular calcium channel blockers TMB-8 (10 μM) and dantrolene (25 μM) [22–25] prior to the perforin incubation. Perforin in a concentration of 2.5 kU/ml induced a transient Ca2+ flux in the pretreated DC (Fig. 4c). Aiming to verify the inhibition of the Ca2+ mobilization from intracellular sources, the DC were subsequently treated with ATP. In TMB-8/dantrolene-pretreated DC ATP did not cause a Ca2+ response, in contrast to the Ca2+ ionophor ionomycin (1 μM), which resulted in a Ca2+ rise (Fig. 4c). The effect of perforin in low Ca2+ buffer was also tested (Fig. 4d). For this purpose Listeria-challenged DC were equilibrated in a low Ca2+ (1.3 μM) buffer before exposure to perforin, which did not result in a Ca2+ response. Only after washout and buffer exchange to normal Ca2+ conditions (1.3 mM), a Ca2+ flux could be provoked by perforin. Comparable to the EthD-2 results above, non Listeria-challenged DC were by a factor 5–10 more sensitive to perforin triggered Ca2+ fluxes (data not shown).
The ability of granulysin to induce Ca2+ fluxes was investigated by incubating granulysin alone at concentrations up to 5 μM, which did not change the intracellular Ca2+ level. Furthermore, simultaneous granulysin and perforin treatment did not increase the response compared to perforin treatment alone (data not shown). These result provide clear evidence that sublytic perforin triggers a transient Ca2+ influx in Listeria-challenged DC. Finally, the role of the transient Ca2+ rise in the granulysin-mediated intracellular bacteriolysis was investigated by the comparison of the enhancing effect of perforin and ionomycin. Ionomycin demonstrated a clear tendency to enhance granulysin-mediated bacteriolysis in all tested samples but due to broader distribution of the single values an overall significance was barely not achieved (p = 0.063) in contrast to the effect of perforin (p < 0.001) (Fig. 4e). The Ca2+ rise induced by ionomycin was furthermore distinguishable from that triggered by perforin as the response was prolonged and the recovery incomplete (Fig. 4f).
Perforin does not influence granulysin binding and initial uptake in DC
To quantify the influence of perforin on granulysin binding and uptake western blot analysis was performed. Following an adapted protocol of Shi et al. , externally bound granulysin was removed by washing with 10 mM arginine to quantify the internalized granulysin fraction. After incubation of DC with granulysin at a concentration of 2.5 μM at 4°C, the arginine washing step removed over 95% of the bound granulysin compared to PBS washing (Fig. 5f). After incubation at 37°C 44% of the total granulysin signal remained detectable following the arginine incubation and was therefore considered as the internalized fraction (Fig. 5g). Co-incubation of perforin in concentrations of 2.5 and 5 kU/ml did not significantly affect the binding of granulysin to DC membranes (Fig. 5f). Granulysin uptake tended to decrease in response to 2.5 kU/ml perforin but the decline was not statistically significant regarding all independent experiments (p = 0.16). A perforin concentration of 5 kU/ml significantly reduced granulysin uptake in human DC (p = 0.009, Fig. 5g).
Perforin does not affect granulysin transfer to early sorting endosomes
Perforin enhances granulysin transfer to Listeria-containing phagosomes
Recently we have shown a perforin-independent pathway of granulysin-mediated bacteriolysis in human DC . Granulysin proved to bind and to be endocytosed in a lipid raft-associated mechanism followed by transfer to L. innocua-containing phagosomes where bacteriolysis was induced. The killing of intracellular Listeria by granulysin was shown to be dose-dependent, but full eradication of the bacteria was not achieved at any applied concentration.
In the current study we were able to demonstrate a significant and robust enhancing role of perforin in granulysin-mediated lysis of intracellular L. innocua in human DC. This enhancing effect could neither be explained by a simple cell loss due to perforin toxicity against the host cells nor by a direct antimicrobial activity of perforin. The observed role of perforin in our experimental system is in agreement with data of other groups describing perforin as a delivering or triggering molecule [8, 13, 14, 27]. For the particular interaction of recombinant granulysin and purified perforin there is just a single study up to now that showed perforin to be essential for granulysin-mediated lysis of M. tuberculosis in human macrophages . However, these results are not fully consistent with the results we obtained in our experimental system using a non pathogenic strain of L. innocua that is killed to some extent by granulysin alone. Furthermore, L. innocua is transferred to lysosomes and killed within 48 hours by the DC itself (data not shown). Mycobacteria like L. innocua used in our system reside in phagosomes of the host cell  but in contrast to L. innocua virulent Mycobacteria have evolved mechanisms to prevent phagosome maturation, especially the fusion with lysosomes to form the lethal phagolysosomes . This active interference of virulent Mycobacteria with the endocytic machinery of the host cell might provide an explanation that granulysin alone does not gain access to the specialized Mycobacteria-containing phagosomes and therefore is not capable of killing the bacteria without perforin.
The triggering role of perforin in the granzyme B-induced apoptosis is, in contrast to the mechanism of granulysin induced bacteriolysis, extensively investigated [14, 27, 30], but underlying mechanisms are still under debate [15, 26, 31]. Similar to granulysin, granzyme B is endocytosed independently of perforin but for induction of the target cell apoptosis it has to gain access to the cytosol. For this delivery step co-treatment of the target cell with perforin is essential . The interaction of granzyme B and perforin is not fully comparable to the findings in our experimental system as we did not find any indication for cytosolic delivery of granulysin in response to perforin but observed enhanced vesicular targeting to L. innocua containing phagosomes.
As perforin was originally described as a pore forming protein we tested its pore forming capability in DC using LDH release assay as well as by the ability to promote the entrance of membrane impermeant EthD-2 or of Ca2+. Perforin in concentrations sufficient for enhanced lysis of intracellular L. innocua resulted in a transient Ca2+ increase but not in a detectable release of LDH or accumulation of EthD-2 in Listeria-challenged DC. The source of the Ca2+ was demonstrated to be the extracellular space as blocking intracellular Ca2+ channels had not effect on Ca2+ waves triggered by perforin or ionomycin. This is further supported by low Ca2+ buffer conditions which abolished perforin induced Ca2+ fluxes. As perforin activity is dependent on free Ca2+, this result might also refer to disturbed perforin membrane binding and multimerization. In our experimental system, no evidence could be provided for a granulysin induced Ca2+ release from intracellular stores as this was reported for higher concentration of granulysin in tumor cells (50 μM, ). These results clearly indicate that sublytic perforin triggers a short-lived disturbance of the plasma membrane permeability not sufficient for significant entrance of a small fluorescent dye but sufficient for a transient Ca2+ influx.
It was coincidentally shown that unchallenged DC were more susceptible to perforin lysis than Listeria-challenged DC. This interesting phenomenon might be explained by recent data showing elevated cathepsin B expression in Toll-like receptor activated DC . Cathepsin B was on the other hand suggested to protect CTL and NK cells from autolysis after degranulation . The protection effect of cathepsin B was called recently into question  and as no further experimental evidence is provided, about mechanisms leading to higher resistance of Listeria-challenged DC against perforin lysis can only be speculated.
In pulse-chase experiments it was demonstrated that enhanced bacteriolysis was still observed when DC were perforin treated up to 25 minutes subsequent to incubation with granulysin. On the other hand, pretreatment of DC with perforin prior to granulysin-mediated listeriolysis had no enhancing effect. These results suggest that stable perforin pores seem not to play a role in promoting augmented passive diffusion of granulysin into target cells. Therefore, the classical pore formation model of perforin allowing delivery of lytic proteins by an increase of membrane permeability is not a major mechanism in granulysin uptake and the induction of enhanced intracellular bacteriolysis. There is a remarkable drop in the enhancing effect, if perforin is first added 75 minutes after pulsing the cells with granulysin. From this result coendocytosis of granulysin and perforin, at least to some extent, can not be excluded to play a role in the enhanced killing of L. innocua in DC. Coendocytosis of granzyme B and perforin to a certain amount was shown to be critical for the induction of target cell apoptosis . The biological role of the transient Ca2+ flux remains to be clarified. Recently, it was shown in HeLa cells that a sublytic perforin concentration triggers via Ca2+ signaling a rapid membrane repair response in the sense of a cellular wound healing system . This process includes the rapid removal of the damaged membrane area from the surface as well as the resealing with intracellular vesicles [36–39]. As a result of this increased membrane turnover in response to perforin, granzyme B is accelerated and augmented endocytosed by target cells . Part of this response is exuberant homotypic and heterotypic membrane fusion, which accelerates phagosome maturation . In another study it was furthermore demonstrated that the inhibition of Ca2+ signaling by Mycobacterium tuberculosis is associated with reduced phagosome-lysosome fusion and crucial for the prolonged survival of the pathogen within phagosomes of macrophages .
To further reveal the mechanism of perforin as an enhancing molecule we studied the impact of perforin on all critical steps of granulysin trafficking in DC, i.e. the binding and initial uptake, the transfer to early sorting endosomes and finally the transmission to L. innocua-containing phagosomes. Sublytic concentrations (2.5 kU/ml) of perforin had no apparent effect on granulysin binding, uptake or transfer to early sorting endosomes. These results are not consistent with a recent study showing that sublytic concentrations of perforin triggers accelerated and enhanced endocytosis of granzyme B as well as transfer to large EEA-1-positive vesicles in HeLa cells . In our experimental system granulysin binding or initial uptake is not the limiting factor for the enhanced induction of bacteriolysis in DC in response to perforin. To the contrary, perforin at a concentration of 5 kU/ml significantly inhibited granulysin uptake in DC. As this perforin concentration is sublytic to DC, the finding of inhibited uptake was unexpected. Because no experimental data is available, it can only be speculated if sublethal damage to DC by perforin inhibits complex cellular processes like endocytosis.
In contrast to binding and initial uptake vesicular targeting of granulysin to L. innocua-containing phagosomes was significantly enhanced by perforin treatment as an indication for improved endosome-phagosome fusion. Early endosomes like all other endocytic organelles can fuse with phagosomes and this fusion process is Ca2+ sensitive [41–44]. We found furthermore some evidence that elevated intracellular Ca2+ indeed plays a role as a signal event promoting enhanced granulysin induced bacteriolysis. The Ca2+ ionophor ionomycin showed a tendency to increase the granulysin mediated intracellular listeriolysis. The mechanism of the intracellular Ca2+ elevation induced by ionomycin is presumably quite different from that induced by perforin which is also reflected in a different shape of the Ca2+ waves with prolonged and incomplete recovery phases. This might explain the inefficient enhancement of ionomycin in comparison to perforin. On the other hand, it is not excluded that perforin triggers additional signalling cascades apart from Ca2+ that are not activated by ionomycin. Finally, we may speculate that sublytic perforin triggers the membrane repair response via Ca2+ signalling. In the course of the membrane repair response endosome-phagosome fusion and thus transmission of granulysin to phagosomes is more likely resulting in enhanced bacteriolysis.
In conclusion, perforin promotes enhanced bacteriolysis by granulysin not by the formation of stable pores that allow passive diffusion of granulysin but rather by an increase in endosome-phagosomes fusion triggered by an intracellular Ca2+ rise.
Production of recombinant granulysin
Recombinant granulysin was produced as previously described . Briefly, a construct corresponding to NKG5 from G 63 to D 132 was cloned in pET28a (Novagen, Inc., WI, USA) containing a c-terminal hexahistidine fusion tag as well as a factor Xa protease cleavage site. A fragment of human β-actin was used as a control protein. Proteins were expressed in Escherichia coli BL21 (DE3) additionally transformed with the chloramphenicol-resistant plasmid, pRARE (Novagen). After lysis of bacteria, granulysin was purified via nickel affinity chromatography, further renatured according to the protocol of Ernst et al. (18) and finally purified using Sep-Pak Vac 6 cc (1 g) C18 cartridges (Waters, Milford, MA, USA).
Purification of perforin and determination of hemolytic activity
Perforin was purified from YT Indy cells according to the protocol of Froelich et al. . Briefly, YT cells were collected by centrifugation, washed twice in Hank's buffered salt solution (HBSS), and resuspended at 108 cells/ml in ice cold relaxation buffer (10 mM PIPES, 0.1 M KCl, 3.5 mM MgCl2, 1 mM ATP, 1.25 mM EGTA, 0.05% BSA, pH 6.8). The cells were disrupted in a nitrogen cavitation bomb (YEDA Scientific Instruments, Rehovot, Israel) at 35 bar at 4°C for 10 minutes. The resulting lysate was centrifuged at 400 × g for 7 minutes and the postnuclear supernatant at 15000 × g for 15 minutes to yield the granule pellet. The granule pellet was extracted by mixing with 1 M NaCl in 20 mM Na-acetate, pH 4.5 containing 2 mM EDTA for 60 minutes at 4°C. After a freeze-thaw cycle the extract was centrifuged at 8,500 × g for 10 minutes. The supernatant was applied to a Econo-Pac 10 DG column (BioRad, Hercules, CA, USA) and eluted with 1 M NaCl, 20 mM HEPES, 10% betaine. The granule extract was purified using cobalt affinity chromatography and eluted by a linear imidazole gradient (0–0.2 M). All gradient fractions were tested for hemolytic activity using a protocol adapted from Henkart et al. . Briefly, dilutions of the fractions in assay buffer (10 mM Hepes, 0.15 M NaCl, and 0.1% BSA, pH 7.5) were incubated with an equal volume of 0.2% human red blood cells (in assay buffer containing 5 mM CaCl2) at 37°C for 20 min in round bottom microtiter plates (Nunc, Rochester, NY, USA). The microtiter plates were centrifuged at 500 × g for 6 min and the supernatants transferred to a second flat bottom microtiter plate. The hemoglobin released into the supernatant was detected with the microplate reader (Spectra MAX 340, Molecular Devices, Sunnyvale, CA, USA) at a wavelength of 420 nm. The fractions containing the highest hemolytic activity were combined and concentrated by ultrafiltration (Centricon, 30 kDa MWCO, Millipore, Billerica, MA, USA) in the presence of EDTA and BSA to yield final concentrations of 2 mM, and 100 mg/ml, respectively. 1 hemolytic unit (U) was defined as the amount resulting in 50% lysis of 0. 1% red blood cells in a volume of 0.2 ml, corresponding to a total amount of 2000000 red blood cells .
Isolation and culture of DC
Human DC were generated in vitro from blood-derived adherent peripheral monocytes as already described . Briefly, human PBMC obtained from venous blood of healthy donors (Blood Bank SRK, Zürich, Switzerland) were isolated by Ficoll-Paque (Pharmacia Biotech, Uppsala, Sweden) density centrifugation. The PBMC were cultured in RPMI 1640 supplemented with penicillin/streptomycin (all Life Technologies, Paisley, UK) and 10% heat-inactivated pooled human A serum (Blood Bank SRK) for 2 h. The adherent cells were cultured for 6 days in DC culture medium composed of RPMI 1640 supplemented with penicillin/streptomycin, 5% heat-inactivated pooled human A serum, rGM-CSF (50 ng/ml, Novartis, Basel, Switzerland), and rIL-4, (100 U/ml, R&D Systems, Abingdon, UK).
Challenge of DC with Listeria
L. innocua were propagated in TSB at 37°C overnight, diluted 10-fold and further expanded to an OD600 of 0.5 corresponding to 5 × 107/ml viable bacteria. Bacteria were harvested by centrifugation, washed twice with PBS prior to opsonization in RPMI 1640 with 50% pooled heat-inactivated human A serum for 30 minutes at 37°C. Opsonized Listeria were washed in PBS and resuspended in RPMI 1640. DC were challenged for 1 hour with a multiplicity of infection (MOI) of 5. Subsequently, cultures were washed with PBS and incubated for 3 hours in DC culture medium containing 25 μg/ml of gentamycin (Sigma-Aldrich, St. Louis, MO, USA) to kill extracellular L. innocua.
Viability determination of L. innocua and DC
Serial dilutions of L. innocua or of L. innocua-challenged DC lysate were spread on tryptic soy broth (TSB; Difco Laboratories, Detroit, MI, USA) agar plates. Colony forming units (CFU) were determined by counting colonies after overnight culture at 37°C and specific lysis was calculated using the formula [(CFU in buffer control - CFU in test incubation)/CFU in buffer control] × 100.
Alternatively, turbidimetry was used to study specific lysis of bacteria . Serial dilutions of treated L. innocua or cell lysates were incubated in 96-well plates (Nunc). Bacterial growth curves were monitored in a microplate reader at OD600 while discontinuous shaking for 16 hours at 37°C. Specific lysis was calculated by determining the time when the maximum population was reached in buffer controls (ODTmax-control). At this time point the OD value (ODTmax-Test) of a shifted growth curve was evaluated and specific lysis was calculated using the formula [(ODTmax-control - ODmin) - (ODTmax-Test - ODmin)/ODTmax-control - ODmin] × 100. All OD values were corrected by subtraction of the baseline OD (ODmin).
Lysis of DC during granulysin and perforin incubation was determined in LDH release assays using the cytotoxicity detection kit (Roche, Basel Switzerland) following the manufacturers instruction. In brief, DC were seeded in a 96-well plate (NUNC) and were challenged with L. innocua in a MOI of 10 prior to treatment with various granulysin and/or perforin concentration for indicated times. For cell lysis analysis 100 μl of cell-free supernatant was harvested, mixed with dye solution, incubated for 20 minutes and absorption was measured at 490 nm. Percent specific lysis was calculated according to the formula: ((experimental value - spontaneous release)/(maximum release - spontaneous release) × 100. Spontaneous release corresponded to untreated DC and cells lysed with Triton-X 100 showed the maximal release.
Bacteriolytic activity of granulysin and perforin
Granulysin in the presence or absence of perforin or perforin alone was incubated at various concentrations for 3 hours at either 4°C or 37°C with Listeria-challenged DC or with 105/ml L. innocua in 0.01 M TrismaR base (pH 8, Sigma-Adrich). Actinfrag, medium or buffer served as controls. For some experiments perforin was replaced by ionomycin in a concentration of 1 μM. After incubation, the viability of L. innocua was determined as described above. Alternatively, induction of listeriolysis was tested using a pulse-chase experimental system. For this purpose, DC were pulsed with granulysin (2.5 μM) for 15 minutes on ice before the medium was replaced and DC further incubated at 37°C. Perforin (2.5 kU/ml) was added at indicated time points for the remaining experimental duration (max. 180 minutes). In addition, some samples were perforin treated for 15 minutes at 37°C prior to medium exchange and further incubation with granulysin for another 180 minutes.
To quantify granulysin binding and uptake L. innocua-challenged DC were incubated with 2.5 μM granulysin and perforin in indicated concentrations for 45 minutes at 37°C or at 4°C, subsequently washed three times for 5 minutes with 10 mM arginine in PBS to remove granulysin bound outside at the cell membrane or PBS alone as control. DC were finally lysed with PBS containing 0.5% Triton-X-100. The content of granulysin bound or internalized in DC was determined by Western blot analysis. Samples were run on a 15% SDS-PAGE gel and blotted onto transfer membranes (Immobilon-P; Millipore). Granulysin was detected using the anti His mAb (1:1000; Invitrogen, Carlsbad, CA, USA). As a reference, cellular actin was detected using an anti-actin mAb (AC15; Sigma-Aldrich). The granulysin content in DC was measured and calculated relative to cellular actin using Image-J software (National Institutes of Health).
Confocal laser scanning microscopy
L. innocua-challenged DC were incubated with various concentrations of granulysin, actinfrag or culture medium alone in presence or absence of perforin for indicated times either at 37°C or at 4°C, subsequently washed twice with PBS and fixed with 1.5% PFA in PBS containing 1% sucrose for immunofluorescence labelling. Fixed DC were scratched and cytospun onto glass slides and permeabilized with 0.1% Triton X-100 (Sigma-Aldrich) in PBS for 1 minute at room temperature (RT). Unspecific binding was blocked with 0.1% BSA bovine serum albumin (BSA; Fluka, Buchs, Switzerland) in PBS for 1 hour RT. Recombinant His-tagged granulysin was detected with a monoclonal anti-His Ab (1:1000). Early endosomes were detected with a rabbit EEA-1 Ab (1:200; Affinity BioReagents, Golden, CO, USA). Omitting the first Abs served as control for specificity. For detection the following Abs were used: FITC-conjugated goat anti-mouse or a goat anti-rabbit Ab (all KPL Inc., Gaithersburg, Maryland, USA), or Texas Red-conjugated donkey anti-mouse Ab (Jackson Immuno Research Laboratories, West Grove, PA, USA). All Abs were diluted in 0.1% BSA in PBS. DNA was labelled with 1 μg/ml DAPI (4,6-diamidine-2-phenyl-indol-dihydrochlorid, Roche, Mannheim, Germany) in PBS for 15 minutes at RT. Fluorescent labelled specimens were examined using a confocal laser scanning microscope (CLSM SP1, Leica, Heidelberg, Germany).
For the detection of plasma membrane pores Listeria-challenged DC were incubated with perforin at the indicated concentration for 45 minutes at 37°C in medium containing 2 μM ethidium homodimer-2 (EthD-2, Invitrogen).
Images were analysed using Imaris software package (Bitplane, Zurich, Switzerland) and threshold levels for calculation of colocalization micrographs (granulysin and EEA-1) were selected above background signals. The degree of colocalization of granulysin with bacterial DNA spots was determined by counting all intracellular distinguishable bacteria as well as those clearly coated by granulysin in at least 200 highly magnified DC per time point.
For measuring intracellular Ca2+, Listeria-challenged or unchallenged DC grown on coverslips were loaded with Fura-2 (Molecular Probes) in a concentration of 10 μM in DC culture medium for 15 minutes at room temperature and were then mounted on a thermostatically controlled chamber maintained at 37°C on an inverted microscope (Zeiss Axiovert 200) equipped with a video-imaging system. For some experiments DC were pretreated with 10 μM dantrolene and 25 μM TMB-8 for 15 minutes at room temperature. Prior to incubation with granulysin and/or perforin in various concentrations and time periods the coverslips were rinsed with incubation buffer (145 mM NaCl, 1.6 mM K2HPO4, 0.4 mM KH2PO4, 5 mM D-Glucose, 1 mM MgCl2, 1.3 mM Ca2+-Gluconate) until stable imaging was achieved. Some samples were rinsed in low Ca2+ buffer (145 mM NaCl, 1.6 mM K2HPO4, 0.4 mM KH2PO4, 5 mM D-Glucose, 1 mM MgCl2, 1.3 μM Ca2+-Gluconate). As positive control for the elevation of intracellular Ca2+ served ATP (1 mM) as well as ionomycin (1 μM). The specimens were excited with light of 340/380-nm wavelengths and the excitations ratio 340/380 was monitored. After certain time periods (30–60 seconds) fluorescent images (Ex 340 nm; Em 525 nm) were recorded.
We are very grateful to Marina Balzer, Gery Barmettler and Mirjam Christen as well as Katja Schulz for excellent technical assistance.
We thank Andreas Schaffner, Markus Schneemann, and Gabriele Schoedon, Medical Clinic B Research Unit, Department of Medicine, University Hospital of Zurich, for providing us with L. innocua. This work was supported by the Hartmann Mueller-Foundation.
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