|Home | About | Journals | Submit | Contact Us | Français|
The immunity-related GTPases (IRGs) constitute an interferon-induced intracellular resistance mechanism in mice against Toxoplasma gondii. IRG proteins accumulate on the parasitophorous vacuole membrane (PVM), leading to its disruption and to death of the parasite. How IRGs target the PVM is unknown. We show that accumulation of IRGs on the PVM begins minutes after parasite invasion and increases for about 1 h. Targeting occurs independently of several signalling pathways and the microtubule network, suggesting that IRG transport is diffusion-driven. The intensity of IRG accumulation on the PVM, however, is reduced in absence of the autophagy regulator, Atg5. In wild-type cells IRG proteins accumulate cooperatively on PVMs in a definite order reflecting a temporal hierarchy, with Irgb6 and Irgb10 apparently acting as pioneers. Loading of IRG proteins onto the vacuoles of virulent Toxoplasma strains is attenuated and the two pioneer IRGs are the most affected. The polymorphic rhoptry kinases, ROP16, ROP18 and the catalytically inactive proteins, ROP5A–D, are not individually responsible for this effect. Thus IRG proteins protect mice against avirulent strains of Toxoplasma but fail against virulent strains. The complex cooperative behaviour of IRG proteins in resisting Toxoplasma may hint at undiscovered complexity also in virulence mechanisms.
Mice deficient in single members of the large family of IFN-inducible immunity-related GTPases (IRG proteins or p47 GTPases) are vulnerable to a number of intracellular pathogens [reviewed in Taylor (2004; 2007;); MacMicking (2005); Martens and Howard (2006)]. The most striking effects have been seen after infection with avirulent strains of Toxoplasma gondii, where to date five IRG proteins have been individually implicated in resistance (Halonen et al., 2001; Butcher et al., 2005; Martens et al., 2005; Ling et al., 2006; Zhao et al., 2009a). There is no consensus about how IRG proteins exercise their resistance function (Howard, 2008). They have been implicated in rapid maturation of the Mycobacterium tuberculosis phagosome (MacMicking et al., 2003), in the initiation of an autophagic process in mycobacterial infection (Gutierrez et al., 2004), and most relevantly to the present paper, in the direct disruption of the T. gondii parasitophorous vacuole membrane (PVM) (Martens et al., 2005; Ling et al., 2006; Melzer et al., 2008; Zhao et al., 2008; 2009a;).
IRG proteins are strongly induced in many cell types by exposure to IFNγ (Boehm et al., 1998). Protein expression can be detected in mouse embryonic fibroblasts (MEFs) 3 h after induction (Boehm, 1999) and reaches a plateau between 24 and 48 h. The proteins distribute among distinct cellular compartments, Irgm1 to the Golgi (Martens et al., 2004) and the endolysosomal compartment (Zhao, 2008; Zhao et al., 2010), Irgm2 to the Golgi (Martens and Howard, 2006; Hunn et al., 2008), Irgm3 (Taylor et al., 1997) and Irga6 (Zerrahn et al., 2002; Martens et al., 2004) to the endoplasmic reticulum (ER). Native Irgb6 and Irgd are predominantly or wholly cytosolic (Martens et al., 2004), Irga6 partitions roughly 60:40 between ER membrane and cytosol, whileIrgm1, Irgm2 and Irgm3 are largely or exclusively membrane-bound (Boehm et al., 1998; Martens et al., 2004; Martens and Howard, 2006). After infection of IFNγ-induced cells with avirulent T. gondii, five out of the six IRG proteins studied were found in high density on the PVM (Martens et al., 2005). We show here that Irgb10 is also found on the T. gondii PVM. Irgm1 has never been reported on the PVM, but accumulates on phagocytic cups and phagosomes in cells phagocytosing M. tuberculosis or latex beads (Butcher et al., 2005; Martens et al., 2005; Shenoy et al., 2007).
It was initially shown in IFNγ-induced primary mouse astrocytes that the T. gondii vacuolar membrane becomes ruffled, vesiculated and ultimately disrupted, exposing the parasite to the cytoplasm, a process dependent on the presence of IRG proteins (Martens et al., 2005), a process since confirmed in mouse astrocytes (Melzer et al., 2008) and peritoneal (Ling et al., 2006) and bone-marrow-derived (Zhao et al., 2008) macrophages and MEFs (Zhao et al., 2009a). Thus the disruption process is not cell type-specific. Recent experiments (Zhao et al., 2009a,b;) strongly suggest that disruption of the IRG-loaded PV is the critical step in T. gondii restriction in IFNγ-induced cells. Disruption of the PV is invariably followed by the death of the parasite and shortly thereafter by the necrotic death of the infected cell (Zhao et al., 2009a). The programme is complete within a few hours of infection and before tachyzoite replication. Virulent T. gondii strains, however, are not efficiently restricted by IFNγ induction, correlated with reduced or absent vacuolar disruption and minimal death of the parasites and host cells (Zhao et al., 2009a). The reduced disruption of vacuoles containing virulent T. gondii is itself correlated with deficient loading of IRG proteins onto the vacuolar membrane (Zhao et al., 2009b,c;).
The process by which IRG proteins access the T. gondii PVM has not previously been subjected to systematic analysis, despite its relevance to the resistance mechanism. We show that loading of IRG proteins onto the PVM begins almost immediately after infection, and rises rapidly for about 1 h. There is a surprising heterogeneity in the intensity of vacuolar loading of IRG proteins, with some vacuoles remaining either completely or almost completely un-loaded. IRG proteins load onto the vacuole in a complex pattern, with Irgb6 and Irgb10 being the most efficient and also the first to load. We seek to explain how IRG proteins make their way from their normal cytoplasmic compartments to the vacuole, and conclude that diffusion from the cytosolic pools, rather than active transport, is the most likely route. Our results confirm a recent report that the autophagic regulator, Atg5, is required for normal loading and suggest that the effect is due to dysregulation of the GTPase cycle of the GKS subset of IRG proteins. Finally, we show that the pattern of vacuolar loading is determined by the strain of T. gondii that inhabits the vacuole. The great majority of PVMs of type I virulent strains are far less intensely loaded with IRG proteins than those of type II or type III avirulent strains in single as well as in co-infections. Because the restriction of virulent strains by IFN-treated cells is far less efficient than the restriction of avirulent strains, the association with vacuolar IRG loading confirms the importance of IRG proteins in resistance of mice to T. gondii, and suggests that they act at the PVM itself. We show that the virulence-associated polymorphic T. gondii kinases, ROP16 and ROP18, as well as a virulence-associated genomic segment containing four related pseudokinases, ROP5A–D, are not individually responsible for virulence-related effect on IRG loading.
IFNγ-induced primary C57BL/6 MEFs were examined for IRG signals at the PVM from 2.5 min up to 2 h after addition of avirulent ME49 T. gondii (Fig. 1A). To increase sensitivity, cells were stained simultaneously with antisera against Irga6 and Irgb6 and detected together. The fastest rise in positive vacuoles occurred 15–30 min after infection, but a few vacuoles were detectably loaded with IRG proteins after 2.5 min. Similar results were obtained when the kinetics of Irgb6 loading were analysed separately as a proportion of IRG-positive PVs over infection time with ME49 T. gondii (Fig. 1B). The increase in number of labelled vacuoles was accompanied by increased intensity of the signals measured at the PVM (Fig. 1C, filled circles and Fig. S1). There was large variation in the intensity of labelling of individual vacuoles that was not diminished when T. gondii infection was synchronized (as described in Experimental procedures) and free parasites were washed off after co-incubation with the target cells (Fig. 1C, open circles).
The rising phase of both the frequency and intensity data may be attributed to variation in the delay associated with loading of individual vacuoles and indeed to some residual asynchrony in the infection. We therefore used time-lapse photography to observe the loading of a transfected EGFP-tagged version of Irga6 (Irga6-ctag1-EGFP) (Zhao et al., 2009a) on to individual PVMs. The time delays before detecting loading were, respectively, 28 min and 9 min in the two frame series shown in Fig. 2A and B (see also Videos S1 and S2). The signal intensities of Irga6-ctag1-EGFP at the PVM in these videos were quantified in consecutive frames (Fig. 2C). Frames from two further videos showing the accumulation of Irgb6-FLAG-EGFP (Fig. S1D) were also quantified (Fig. 2C, Irgb6 I and II). The four data sets illustrate two independent contributions to the rise in loaded vacuoles shown in Fig. 1. First, there is variation in the time of entry of the T. gondii into the cell, which can be as early as the first minute or two in the Irga6 I series (Fig. 2A) but also as late as 60 min in the Irga6 II series (Fig. 2B). Second, there is heterogeneity in the length of the delay after infection before loading begins, which can be as short as 2.5 min in rare vacuoles seen in the fixed preparations (Fig. 1), and in one of the quantified Irgb6 videos (Fig. 2C, Irgb6 I), 9 min in Irga6 II (Fig. 2B and C) and as much as 28 min in Irga6 I (Fig. 2A and C). Once IRG accumulation is initiated it rises roughly linearly for 30–60 min.
The combined intensities of vacuolar accumulation recorded for Irga6 and Irgb6 during the first 2 h after infection were remarkably heterogeneous (Fig. 1C). We analysed pixel intensities of Irga6 and Irgb6 independently at the PVM in MEFs induced for 12–48 h with IFN and infected for a further 2 h with T. gondii (Fig. 3A and B). Absolute levels of Irgb6 and to a lesser extent Irga6 protein in the cells increased with time after IFNγ stimulation (Fig. 3C). Sixty intracellular vacuoles were quantified per time point for Irga6 and Irgb6. The great majority of vacuoles accumulated some IRG protein but the amount accumulated varied from very high values all the way down to the visible threshold and below. The mean expression of Irga6 and Irgb6 increased up to 48 h after IFN induction (Fig. 3C) as did the IRG protein level on the 2 h post-infection PVM (Fig. 3A and B), suggesting that IRG protein accumulation on the vacuole is partly concentration-driven. So heterogeneity in IRG protein level in individual cells could contribute to heterogeneity of PVM loading. Nevertheless most of the observed heterogeneity is evidently intrinsic to the individual vacuole. This could be visualized directly for the cell shown in Fig. 2B (Video S2), which is already infected with one T. gondii (arrow) before a second one enters (arrowhead). The PVM of the first parasite already has clear Irga6-ctag1-EGFP accumulation that does not change during the video while the accumulation on the PVM of the second T. gondii rapidly overhauls the first one and becomes very bright. Some vacuoles remained free of IRG protein for hours: other vacuoles in the same cell could be heavily loaded. The nature of this vacuole-specific heterogeneity in IRG loading is obviously of interest as it relates directly to the ability of individual parasites to escape attack by IRG resistance proteins.
Transfer of Irga6 to the T. gondii PVM shortly after infection in IFNγ-induced cells is associated with GTP binding (Hunn et al., 2008; Papic et al., 2008) raising the possibility that activation of Irga6 results from the receipt of a cellular signal stimulated by infection. However disruption of major signalling systems failed to prevent the loading of IRG proteins onto the vacuoles of infecting T. gondii. We used wortmannin and Ly294002 to inhibit PI3 kinases, pertussis toxin to inhibit signal transmission from G protein-coupled receptors, MyD88-deficient MEFs to investigate a possible role of signalling through Toll-like receptor (TLR) signalling pathways and z-VAD-fmk to inhibit activation by caspases (see Experimental procedures for details). In no case was there any effect on the transfer of either Irga6 or Irgb6, analysed separately, to the PVM (Fig. 4; for controls see Fig. S2A and B). Irga6 has been reported to interact with Hook3, a Golgi-associated microtubule binding protein (Kaiser et al., 2004) but dissociation of the microtubule network by nocodazole had no effect on the accumulation of IRG proteins at the PVM (Figs 4 and S2C). It therefore seems likely that transfer of IRG proteins to the vacuole is mediated by diffusion from the cytosolic pools of these proteins (Martens et al., 2004; Martens and Howard, 2006) and activation of IRG proteins by GTP binding probably occurs at the PVM (Hunn et al., 2008; Papic et al., 2008).
IFNγ-induced mouse fibroblasts lacking the autophagic regulator, Atg5, restrict growth of avirulent ME49 strain of T. gondii weakly (Könen-Waisman and Howard, 2007), and Atg5-deficient macrophages stimulated with IFNγ and LPS are deficient in accumulating Irga6 at the PVM of the type II avirulent PTG strain of T. gondii (Zhao et al., 2008). Figure 5A confirms for MEFs that significantly fewer ME49 vacuoles in the Atg5-deficient cells load with Irga6. In addition, the loading intensity of individual vacuoles with Irga6 was somewhat reduced (Fig. 5B). Loading of Irgb6 was greatly reduced in Atg5-deficient cells, and that of Irgd almost absent, showing that the lesion is not specific for Irga6 (Fig. 5A and B), but includes all three proteins of the GKS subfamily. The cellular levels of these IRG proteins were also reduced, especially so for Irgb6 and Irgd (Fig. 5C). Levels of the GMS subfamily proteins, Irgm1 and Irgm3, on the other hand were normal in Atg5-deficient fibroblasts. A slight reduction in Irgm2 may be attributed to the allele specificity of the antiserum used for its detection (see Experimental procedures). Like Zhao et al. (Zhao et al., 2008), we noted that Irga6 was at least partially distributed in small aggregates in IFNγ-induced Atg5-deficient cells. These aggregates were stained with the monoclonal antibody, 10D7, specific for a conformation of Irga6 associated in vivo with the binding of GTP (Papic et al., 2008) (Fig. 5D upper panels). Irgb6 and Irgd were also found in aggregates (Fig. 5D middle and lower panels). Proximity of Irga6 aggregates with LAMP1 in Atg5-deficient macrophages observed by Zhao et al. (Zhao et al., 2008) was not seen in Atg5-deficient fibroblasts (Fig. S3).
Each IRG protein accumulates on a characteristic proportion of vacuoles. Thus Irga6 and Irgb6 both load onto the majority of vacuoles (Figs 1–5) (Martens et al., 2005; Hunn et al., 2008; Papic et al., 2008), but Irgb6 invariably loads onto a higher proportion of vacuoles than Irga6 (Figs 4 and 5A). By discriminating two or three IRG proteins at a time on single intracellular parasites we examined the proportions of loaded vacuoles, as well as the coupled or uncoupled distribution, of Irga6, Irgb6, Irgb10, Irgd, Irgm2 and Irgm3. All antibody reagents used showed saturation binding to their vacuolar targets (Fig. S4 and A. Khaminets and S. Könen-Waisman, unpublished data). Four different immunoreagents failed to find any vacuolar loading of Irgm1, despite its strong association with resistance to T. gondii (S. Könen-Waisman, unpublished data and see also Martens et al., 2005). Vacuolar loading by five IRG proteins fell into a consistent hierarchy in the order Irgb6 > Irgb10 > Irga6 > Irgm2 ≈ Irgd (Fig. 6A). Irgm3 frequency was low, probably below Irgd/Irgm2, but a value is not shown because the loading intensity was low and difficult to resolve from the surrounding ER. The hierarchy was reproducible except for the relative positions of Irgd and Irgm2 and was independent of the reagents used.
If IRG proteins load randomly onto vacuoles, then essentially every vacuole should be loaded with one or the other and most with more than one in random combinations. However when the loading of two or more members of the family was scored on each vacuole it was clear that they were strongly correlated. In Fig. 6B this is illustrated for pairs of IRG proteins at different positions in the loading hierarchy. Invariably, vacuoles loaded with the IRG protein lower in the hierarchy are very largely or completely included in the set of vacuoles loaded with the IRG protein higher in the hierarchy (The full data from which Fig. 6B was generated are given in Table S1). Thus 98.4% (612/622) of vacuoles loaded with Irga6 were also loaded with Irgb6, while 100% (390/390) of vacuoles loaded with Irgd were also loaded with Irga6 (Fig. 6B and Table S1). The two highest members of the hierarchy, Irgb6 and Irgb10 were about 90% correlated. The effect of the correlated loading of IRG proteins is that a significant number of vacuoles (normally 10–20%) did not load with any IRG proteins at all while about 40% of the vacuoles (i.e. those loaded with Irgd or Irgm2) were loaded with all the IRG proteins studied.
The correlated loading behaviour suggested that IRG proteins might assemble on the vacuoles in sequence. Analysis of Irga6 and Irgb6 accumulation on to ME49 T. gondii strain vacuoles in double-labelled samples taken shortly after infection showed that the earliest increase in label is due to accumulation of Irgb6, followed several minutes later by Irga6 (Fig. 6C). Live cell observation confirmed this result for Irgd, which loaded later than Irgb6 or Irga6. ME49 strain vacuoles were observed in IFNγ-induced MEFs transfected with Irgd-ctag1-Cherry together with either Irgb6-FLAG-EGFP (Fig. 6D) or Irga6-ctag1-EGFP (Fig. S5). Invariably the IRG protein higher in the hierarchy was the first to load, followed after a variable delay of several minutes by the lower member (Fig. 6D, Irgb6 followed by Irgd; Fig. S5, Irga6 followed by Irgd). In no case were vacuoles found to load with the lower member first.
In Irga6-deficient MEFs (Martens et al., 2005) the loading of Irgd to Irgb6-positive vacuoles was not affected. The hierarchical series formed as usual, but without Irga6 (Fig. 6E). The inclusion relationships described above were also preserved in Irga6-deficient cells (S. Könen-Waisman, unpublished data). There was, however, a numerically highly significant tendency (P < 0.0001 by Mann–Whitney test) towards reduced Irgb6 vacuole loading intensity in Irga6-deficient cells relative to the wild-type (wt) cells (Fig. 6F), suggesting that the presence of Irga6 may stabilize the loading of Irgb6. No effect on that scale was seen for Irgd or Irgm2 (Fig. 6F).
The three GMS proteins, Irgm1, Irgm2 and Irgm3, characterized by a unique substitution of methionine for lysine in the G1 motif of the nucleotide-binding site (Boehm et al., 1998), control the GTPase cycle of the conventional GKS proteins, Irga6, Irgb6 and Irgd (Hunn et al., 2008). In the absence of the GMS proteins, Irga6 and Irgb6 form nucleotide-dependent cytoplasmic aggregates that are probably caused by premature GTP binding and activation (Hunn et al., 2008; Papic et al., 2008). Irga6, expressed alone in 3T3 cells from a Mifepristone-inducible construct, was unable to relocate to the PVM of infecting T. gondii strain, but vacuolar location was restored if the three GMS proteins were also introduced by transfection (Hunn et al., 2008). However the frequency of Irga6-loaded vacuoles was low (Hunn et al., 2008) and accumulation of Irga6 at the PVM was weak (Fig. 7 and J.P. Hunn, unpublished data). The co-ordinated loading described above hinted that Irgb6 (and/or other GKS proteins) might be necessary for complete loading of Irga6. We therefore reconstituted Mifepristone-induced gs3T3-Irga6 fibroblasts with constructs expressing Irgb6, Irgd or both as well as the three GMS proteins and determined the Irga6 signal intensity on T. gondii PVM 2 h after infection. Coexpression of either Irgb6 or Irgd or both caused a significant increase in the Irga6 signal at the PVM without increasing the frequency of Irga6-loaded vacuoles (Fig. 7, Hunn et al., 2008 and J.P. Hunn, unpublished data). Thus other IRG proteins of the GKS group are required for efficient Irga6 loading of the PVM. Unlike Irga6, Irgd does not load at all on to the PVM if only the three GMS proteins are also present, but loads if Irgb6 is also present (J.P. Hunn, unpublished data). Thus the loading of the PVM by GKS proteins is a highly cooperative process, with Irgb6 and probably also Irgb10 arriving as pioneers and subsequently becoming stabilized by the arrival of Irga6 and Irgd. In this context, it may be significant that both Irgb6 and Irgb10 can load, albeit inefficiently, onto T. gondii vacuoles in the absence of other IRG proteins (Hunn et al., 2008, Fig. 7 and J.P. Hunn, unpublished data). A different explanation for the presence of Irgm2 and Irgm3 at the vacuole is presented in the Discussion.
Reduced loading of Irgb6 on virulent type I strain RH PVs has recently been reported in MEFs and macrophages, correlating with reduced vacuolar disruption (Zhao et al., 2009a,b,c;). The data shown above were all based on infection of cells with the avirulent T. gondii strain, ME49. As shown in Fig. 8A, two type I strains, BK and RH, gave grossly defective loading of Irgb6, while two avirulent type II strains, ME49 and NTE, and an avirulent type III strain, CTG, showed the familiar high frequency of Irgb6-loaded vacuoles. Loading of all IRG proteins was attenuated on RH strain vacuoles (Fig. 8B) but two different effects were apparent. Irgb6 and Irgb10 loaded onto very few vacuoles, while for Irga6 or Irgd the number of loaded vacuoles was significantly but not dramatically reduced but the amount loaded per vacuole was generally much lower, documented for Irga6 in Figs 8C and D and S6. The few vacuoles loaded with Irgb6 were loaded very heavily (Fig. 8C and D) and were additionally all intensely loaded for Irga6 (Figs 8E and S6) and Irgd (J.P. Hunn and S. Könen-Waisman, unpublished data). In addition to their implications for the nature of virulence, these results also support the concept that Irgb6 and Irgb10 function as loading pioneers. In their absence, the remaining IRG proteins have difficulty gaining a foothold on the vacuole. In IFN-induced MEFs co-infected with RH-YFP and unlabelled ME49, ME49-containing vacuoles could be intensely coated with Irgb6 while RH-containing vacuoles in the same cell had none (Fig. 8F), and the loading intensity of Irgb6 and Irga6 on ME49 PVs was unaffected by the presence of RH-YFP vacuoles (Fig. 8G). It is therefore unlikely that a diffusible molecule from the virulent strain is responsible for reduced Irgb6 loading. Our results and conclusions confirm those of Zhao et al. (Zhao et al., 2009c).
Polymorphic T. gondii genes encoding rhoptry kinases and pseudokinases of the ROP2 family secreted into the host cell at the point of entry (Carruthers and Sibley, 1997) contribute to the differential virulence phenotypes of T. gondii types I, II and III strains (Saeij et al., 2006; Taylor et al., 2006; El Hajj et al., 2007a). ROP18 accumulates on the PVM of the invading parasite and ROP18 expressed in infected cells by transfection also targets the PVM (El Hajj et al., 2007a). ROP18 differs in amino acid sequence between all three virulence types (Saeij et al., 2006) and is under-expressed in avirulent type III parasites. However expression by transfection of mature form ROP18 from the virulent RH strain into IFNγ-induced L929 fibroblasts had no effect on the number of ME49 vacuoles loaded with Irgb6 compared with cells expressing either ME49-derived ROP18, or Cherry as a transfection control (Fig. 9A).
Two further polymorphic ROP2 family members have been implicated in virulence-related behaviour. ROP16 alleles differentially affect cellular signal transduction pathways responsible for inflammation in vivo (Saeij et al., 2007) and have some impact on virulence (Saeij et al., 2006), while a virulence QTL on Chromosome XII embraces the ROP5 locus (Saeij et al., 2006). This locus, originally annotated as a single gene called ROP5 (TGME49_108080), contains five nearly identical ROP2 family members dubbed ROP5A–E (http://www.toxodb.org and J.C. Boothroyd, unpublished data; Saeij et al., 2006). We assayed the loading of Irgb6 onto the PVMs of virulent RH strain deficient in ROP16 (RH-Δrop16) compared with the RH wt control, and onto the PVMs of an avirulent strain, S22, transgenic for cosmid LC37 (S22-LC37) carrying a segment of the RH genome encompassing ROP5A–D as well as two other predicted gene sequences (TGME49_108070 and TGME49_108060). Neither genetically modified parasite was affected in its behaviour vis-à-vis the IRG resistance mechanism (Fig. 9B). RH-Δrop16 showed the same deficit in Irgb6 loading as the wt virulent RH strain. Likewise, T. gondii S22-LC37 behaved no differently from the avirulent parental S22 strain (Fig. 9B and S. Könen-Waisman, unpublished data). RH-Δrop16 replication was no better controlled by IFNγ treatment of the host MEFs than RH itself, while S22-LC37 was as well controlled by IFNγ as parental S22 (Figs 9C and S7).
The PVM of T. gondii parasites infecting IFNγ-induced mouse cells becomes coated with multiple members of the IRG family of IFN-inducible resistance GTPases. The process is important for resistance because IRG proteins are able to disrupt the PVM (Martens et al., 2005), and vacuolar disruption leads to the rapid death of the enclosed parasite (Zhao et al., 2009a). The IFNγ-dependent resistance mechanism largely fails when the infecting T. gondii is a virulent type I parasite (Zhao et al., 2009a,b,c;). We show here that this is because IRG proteins fail to load effectively on to the PVM. To understand the mechanistic basis for T. gondii virulence and avirulence in mice, we have therefore begun to dissect the process by which IRG proteins load on to the PVM.
The earliest infecting parasites begin to accumulate IRG proteins on the PVM within 2.5 min of addition to culture, but the proportion of IRG-loaded vacuoles rises for about 1 h (Fig. 1A). There is a delay of highly variable length before IRG proteins begin to accumulate (Fig. 2) but once initiated, IRG protein accumulation is roughly linear for up to 1 h (Fig. 2C). Cytoplasmic Irga6 molecules areprobably GDP-bound while those that accumulate on the PVM are GTP-bound (Hunn et al., 2008; Papic et al., 2008). Extensive GTP-dependent interactions between IRG protein molecules, documented elsewhere (Hunn et al., 2008) and in the present study, would allow for the formation of homo- and hetero-oligomers at the PVM. The variable delay in initiating loading suggests that the rate-limiting step for colonization of the PVM is the initiation of oligomerization by GTP binding at the PVM. Once oligomerization begins, further molecules of GTP-bound IRG proteins can be added with high efficiency.
Our experiments indicate that the transfer of IRG proteins to the PVM is not triggered, for example by phosphorylation, via the main cell-signalling systems activated by infection (Figs 4 and S2). No effect was seen following inhibition of classical PI3 kinases, of G protein-coupled receptors, of caspases, or by removal of the MyD88 adaptor of TLR signalling even though the TLR system is stimulated by several independent Toxoplasma elicitors (reviewed in Egan et al., 2009). We have, however, not yet explored the possibility of a trigger emanating from a TLR via a MyD88-independent pathway or from a cytoplasmic detector such as one of the NALP proteins.
The microtubule cytoskeleton is not directly involved in transporting IRG proteins to the PVM, despite evidence that Irga6 interacts with the microtubule binding protein, Hook3 (Kaiser et al., 2004) as nocodazole treatment failed to block vacuolar loading by Irga6 or Irgb6 (Fig. 4 and Fig. S2). Thus the infection process probably does not trigger the activation or active transport of IRG proteins via a host mechanism. We suggested recently that the characteristics of the Toxoplasma vacuolar membrane directly stimulate the re-localization of IRG proteins (Hunn et al., 2008). The key issue is: why do IRG proteins concentrate on this membrane? All the GKS proteins, including the pioneer, Irgb6, could initially reach the PVM by simple diffusion as they have large cytosolic pools (Martens et al., 2004). It is not yet known how Irgb6, lacking evident membrane attachment signals, associates with PV membranes. Perhaps an early interaction with Irgb10, which has a perfect myristoylation motif (Bekpen et al., 2005), assists Irgb6 targeting. Myristoylation of Irga6 is essential for its own vacuolar targeting (N. Papic, unpublished data). However to avoid premature activation on endogenous cellular membranes the GKS proteins require the presence of all three of the membrane-bound GMS proteins (Hunn et al., 2008), which are distributed differentially on Golgi, ER (Taylor et al., 1997; Martens et al., 2004; Martens and Howard, 2006) and lysosomal membranes (Zhao et al., 2010). The initial absence of GMS proteins on the PVM immediately after infection may therefore provide a window for spontaneous activation at this membrane.
There is remarkable variation in loading intensity even within single cells for both Irga6 and Irgb6 (Figs 1C and 3A and B), with some vacuoles apparently failing completely to acquire any IRG proteins over many hours (Fig. 2C, Video S2 and Y.O. Zhao, unpublished data). Vacuoles may become progressively more resistant to IRG loading with time after infection, perhaps through the maturation of a parasite-determined defence mechanism. Such an effectcould be related to the mechanism of virulence discussed below.
Our data (Fig. 6A and B and Table S1) establish that different IRG proteins assemble cooperatively on the PVM in a distinct order, with Irgb6 and Irgb10 as pioneers. If vacuoles become resistant to IRG loading with time after infection, then this process probably affects the loading of Irgb6 and Irgb10. The strong cooperativity of loading would thereby ensure that a proportion of vacuoles would remain free of IRG proteins. We have shown recently that all three GMS proteins, Irgm1, Irgm2 and Irgm3, are required for loading of Irga6 onto the PVM of ME49 strain T. gondii (Hunn et al., 2008). However this loading is inefficient unless other GKS proteins, Irgb6 and/or Irgd, are also present (Fig. 7). The present study confirms this, as nearly all Irga6-loaded vacuoles were also positive for Irgb6 and Irgb10 (Fig. 6B and Table S1). Finally, Irga6 loading of Irgb6-negative vacuoles containing the virulent RH strain is far less efficient than the loading of the rare Irgb6-positive vacuoles (Fig. 8). These results suggest that Irga6 accumulation is directly facilitated or stabilized by the presence of Irgb6 and Irgd, and, we anticipate, of Irgb10 as well. This effect may well be due to the formation of mixed GTP-dependent oligomers because at least Irga6 and Irgb6 interact strongly in a nucleotide-dependent manner in yeast 2-hybrid assays (Hunn et al., 2008). That stabilizing interactions are reciprocal is suggested by the highly significant reduction in Irgb6 signal at the PV (P < 0.0001) in the absence of Irga6 (Fig. 6F). We conclude that Irgb6 and probably also Irgb10 are ‘pioneers’ in being able to load at least to some extent by themselves. Their loading is then reinforced by the arrival of the other GKS proteins. Because Irgd loading is not detectably affected by loss of Irga6, Irgd either normally does not interact with Irga6 on the vacuole or alternatively in the absence of Irga6 it interacts with other members of the hierarchy. There is at present no reason to favour either of these alternatives over the other.
Whether such thinking is appropriate for the association of the regulatory GMS proteins with the PVM is not clear. The GMS proteins have low (Irgm2, Irgm3) or absent (Irgm1) free cytosolic pools (Martens et al., 2004; Martens and Howard, 2006) so access to the vacuole by free diffusion is limited. Irgm3 is associated with the ER membrane, and Irgm3 association with the PVM could be due to the investment of the PV by ER cisternae (Melzer et al., 2008) or by direct fusion between PV and ER membranes (Goldszmid et al., 2009). Irgm2 is exclusively associated with Golgi membranes (Martens and Howard, 2006), but a secondary association with the PVM via Golgi-ER exchange is possible. However Irgm1, with no cytosolic pool (Martens et al., 2004), is also associated prominently with the Golgi (Martens et al., 2004; Butcher et al., 2005), but is never detected on the PVM. The GMS proteins are essential regulators of the GKS subfamily, maintaining these latter in the GDP-bound state before infection probably by direct GDP-dependent interaction (Hunn et al., 2008). After infection, the PVM is a site of highly concentrated GKS proteins, initially in the GTP-bound state, but presumably exerting their function at the vacuole via GTP hydrolysis. Thus the Irgm2 and Irgm3 proteins found at the vacuole may reflect binding of the small cytosolic pools of these proteins to PVM-localized GKS molecules that have hydrolysed their GTP to GDP but have not dissociated from the vacuole. This model is consistent with the absence of Irgm1 from the PVM and with the dependence of PV binding of both Irgm2 and Irgm3 on the presence of GKS proteins (Hunn et al., 2008).
C57BL/6 mice possess other GKS proteins that we have not yet analysed in detail (Bekpen et al., 2005). We have, however, indications that some of these also associate with avirulent T. gondii vacuoles (J.C. Howard and R. Lange, unpublished data). How these will fit into the loading hierarchy remains to be seen.
In view of IRG function in T. gondii resistance it is of great interest whether intense loading of PVs with multiple IRG proteins favours PVM vesiculation and parasite death. Although critical experiments are still missing, the correlation between reduced PV loading with IRGs and reduced vacuole disruption in virulent T. gondii infection indicates that this might indeed be the case. Furthermore, control of T. gondii is somewhat reduced in Irga6-deficient cells (Martens et al., 2005) and in vivo in Irgd-deficient mice (Collazo et al., 2001). Thus the significance of multiple IRG protein loading seems to be reflected in the non-redundancy of the two GKS proteins that have been knocked out so far.
IFNγ-induced mouse fibroblasts lacking the autophagic regulatory protein, Atg5, do not control avirulent T. gondii replication efficiently (Könen-Waisman and Howard, 2007) and Irga6 fails to load the PV in Atg5-deficient macrophages, forming cytosolic aggregates (Zhao et al., 2008). Thus Atg5 may have a specific function in loading Irga6 onto the PV. However, we find in Atg5-deficient fibroblasts that defect in vacuolar loading involves all the tested GKS proteins (Fig. 5). Not only Irga6 but also Irgb6 and Irgd formed aggregates in the Atg5-deficient IFNγ-induced fibroblasts, and the Irga6 aggregates bind the GTP-dependent monoclonal antibody 10D7 (Fig. 5) (Papic et al., 2008). GTP binding by the GKS subfamily of IRG proteins is normally controlled by dynamic interactions with the GMS subfamily (Hunn et al., 2008), and when such control is lost, Irga6 and Irgb6 form GTP-dependent aggregates in the cytosol and do not localize to the PVM (Hunn et al., 2008; Henry et al., 2009a). Furthermore, the reduction in GKS protein levels in Atg5-deficient cells (Fig. 5) recalls the reduced GKS protein levels found in IFNγ-induced cells from Irgm1- and Irgm3-deficient mice (Henry et al., 2009a). Taken together we conclude that Atg5 has an effect on IRG protein loading onto T. gondii PV, but that this is indirect as absence of Atg5 causes inappropriate activation of the GKS proteins resulting in their mislocalization and aggregation and presumably subsequent degradation. Our findings suggest that Atg5 expression may be necessary for the normal function of the three GMS proteins in regulating nucleotide exchange in the GKS subfamily on the membranes of cytoplasmic compartments (Hunn et al., 2008). Which if any of the increasing range of activities attributed to Atg5 (Hanada et al., 2007; Geng and Klionsky, 2008) could be responsible for this activity is unclear.
Reduced loading of IRG proteins onto the vacuoles of virulent strains was recently reported by Zhao et al. (Zhao et al., 2009c) in activated mouse peritoneal macrophages. They did not report the minority of vacuoles with heavy IRG loading seen here in fibroblasts (Fig. 8C–E), perhaps reflecting the two rather different cellular systems. The failure of IRG loading on the great majority of vacuoles derived from virulent T. gondii strains (Fig. 8) suggests specific inhibition by the parasite. Irgb6 and Irgb10 are most affected, the two proteins that load earliest and most efficiently on vacuoles of an avirulent strain (Fig. 6). Targeting of Irgb6 and Irgb10 would be an economical defence strategy against IRG proteins, as in their absence vacuolar loading by other IRG proteins becomes inefficient. The inhibition of Irgb6 loading by the virulent strain, although striking, is not complete. Approximately 10% of vacuoles load heavily with Irgb6 and Irga6 and behave like the IRG-loaded vacuoles of an avirulent strain (Zhao et al., 2009a): they disrupt, the parasite dies and the infected cell subsequently dies by necrosis (Y.O. Zhao, unpublished data). We proposed above that the failure of a proportion of vacuoles to load with IRG proteins even during infection with avirulent T. gondii could be due to some form of maturation towards resistance to IRG loading induced by the parasite. An exaggerated or accelerated form of the same process could account for the situation with virulent strains.
The fact that inhibition is not dominant in mixed infections with virulent and avirulent strains (Fig. 8F and G) suggests that the inhibitory effect is mediated directly at the vacuolar membrane. Our experiments argue against a role for the rhoptry proteins, ROP5, ROP16 and ROP18 in this effect, although all three have been implicated genetically in virulence differences between T. gondii strains. For ROP18, our results (Fig. 9) confirm for fibroblasts what was reported recently by Zhao et al. for macrophages (Zhao et al., 2009c). ROP18 seemed initially a good candidate because it associates with the PVM and is an active kinase. However both sequence and expression results group types I and II strains alleles together with type III alleles as the outlier, while IRG-related virulence effects group the avirulent types II and III strains together with type I as the outlier. Unlike ROP18, ROP16 is not localized at the PVM, has a known action on host inflammatory kinases and is associated with only modest mouse mortality in genetic tests (Saeij et al., 2006; 2007;). Additionally, the ROP16 alleles of types I and III strains confer an indistinguishable phenotype in STAT activation assays and are nearly identical at the protein level (Saeij et al., 2007). Like ROP18, the ROP5 genes encode ROP2 family members associated with the PVM (El Hajj et al., 2007b) but none of the five ROP5 genes appears to encode a catalytically active kinase (El Hajj et al., 2006 and J.C. Boothroyd, unpublished data). By the IRG-related assays described here S22-LC37, carrying four of the five ROP5 alleles of the RH strain, behaves like the avirulent parental S22 strain. In addition, the types I and III alleles for the entire ROP5A–E cluster are highly similar while type II and III, which are similar in IRG recruitment, carry very different versions of this cluster (toxodb.org and J.C. Boothroyd, unpublished data). Thus none of the tested ROP proteins are strong candidates a priori for the virulence-associated IRG loading effects. Further genetic studies will surely reveal the T. gondii genes involved.
IRG proteins are major players in T. gondii resistance in mice and show a high degree of cooperative activity (Hunn et al., 2008 and this paper), consistent with their non-redundancy in single gene knockouts. Because T. gondii virulence is also determined by epistatic interactions between alleles at multiple loci (Saeij et al., 2006) the single-locus gain-and-loss cases analysed here may fail to reproduce the complexity of the natural situation.
Toxoplasma gondii is not the only organism where virulence differences are associated with the mouse IRG system. The human pathogen, Chlamydia trachomatis, is resisted by interferon-induced mouse cells through the action of at least three IRG proteins, Irgm1, Irgm3 and Irgb10 (Bernstein-Hanley et al., 2006; Miyairi et al., 2007; Coers et al., 2008) while the mouse-specific race, Chlamydia muridarum is not controlled. Control of C. trachomatis and lack of control of C. muridarum is correlated with the presence or absence of IRG proteins, specifically Irgb10, on the Chlamydia inclusion (Coers et al., 2008). C. muridarum and C. trachomatis are over 90% identical at the nucleotide level and share over 99% of their open reading frames (Stephens et al., 1998; Read et al., 2000), while virulent type I and avirulent types II and III T. gondii clonal lineages are greater than 95% identical at the nucleotide level (Boyle et al., 2006), thus facilitating in both cases the search for loci responsible for these large differences in virulence. Probably when the resistance mechanisms of the virulent strains of both parasites are revealed they will contribute to the elucidation of the IRG resistance mechanism itself.
The loading of multiple IRG proteins onto vacuolar inclusions has been documented for only two intracellular organisms, T. gondii and C. trachomatis. Mice deficient in several individual IRG proteins show susceptibility phenotypes to these pathogens. However, IRG-dependent resistance in mice has been claimed for many other protozoal and bacterial pathogens based always and only on mice deficient in Irgm1, the GMS subfamily regulator protein that does not localize to the T. gondii vacuole (Martens et al., 2005; Taylor, 2007). Because Irgm1 has been shown to relocate to phagocytic cups and phagosomes during particle uptake (MacMicking et al., 2003; Martens et al., 2004) it has been proposed that this IRG protein can implement a direct cell-autonomous attack on phagocytosed pathogens (MacMicking et al., 2003). However, Irgm1 deficiency is associated with haemopoietic stem cell failure (Feng et al., 2008), defective proliferative potential of T lymphocytes in animals infected with highly immunostimulatory parasites such as Mycobacteria (Feng et al., 2004; Santiago et al., 2005) and with cell-autonomous anomalies of macrophage behaviour (Henry et al., 2007; 2009b;). Thus susceptibility of Irgm1-deficient mice to multiple organisms may follow from the immunodeficiency rather than from loss of a direct action by Irgm1 against pathogen inclusions of various kinds. Indeed, the complex deficiency of the Irgm1-deficient mouse is completely reversed in the Irgm1/Irgm3 double-deficient mouse (Henry et al., 2009a), showing that neither the presence of Irgm1 nor of Irgm3 is in fact required for resistance to the ‘Irgm1-dependent’ organisms such as Salmonella or Mycobacteria. The evidence now suggests that the generalized, IFNγ-dependent immunodeficiency caused by loss of Irgm1 is due to loss of one of the three essential regulator proteins of the IRG system, and probably results from the cytopathic effects of activated GKS subfamily IRG protein aggregates in the cytoplasm (Hunn et al., 2008; Papic et al., 2008; Henry et al., 2009a). This complex conclusion shows how important it is to study the interacting components of the IRG system in order to understand the implications of single IRG gene knockout data. Resistance to T. gondii does not follow the Irgm1 paradigm as the Irgm1/Irgm3 doubly deficient mouse is highly susceptible to the pathogen (Henry et al., 2009a). Thus resistance to T. gondii (and presumably also C. trachomatis) is truly dependent on the integrity of the IRG system. An issue for the future is to understand what the T. gondii and C. trachomatis vacuoles have in common that makes them targets for IRG protein action.
The following mammalian expression constructs were used: pEGFP-N3-Irga6-ctag1, pmCherry-N3 (both from Zhao et al., 2009a); pGW1H-Irgm1 (Martens et al., 2004); pGW1H-Irgb6-FLAG, pGW1H-Irgm2, pGW1H-Irgm3 and pGW1H-Irgd (all from Hunn et al., 2008). pmDsRed-N3-Irgb6-FLAG was made via PCR amplification of Irgb6-FLAG from pGW1H-Irgb6-FLAG construct using the following primers: forward 5′-cccccccccgtcgaccaccatggcttgggcctccagc-3′ and reverse 5′-cccccccccgtcgaccttgtcatcgtcgtccttgtaatc-3′ and insertion into pmDsRed-N3 (Zhao et al., 2009a) following SalI digestion. pEGFP-N3-Irgb6-FLAG was generated by subcloning Irgb6-FLAG fragment from pmDsRed-N3-Irgb6-FLAG into pEGFP-N3 (Clontech) using SalI digestion. pmCherry-N3-Irgd-ctag1 was generated by PCR amplification of Irgd-ctag1 from pGW1H-Irgd-ctag1 (Hunn et al., 2008) using the following primers: forward 5′-ccccccgtcgaccaccatggatcagttcatctcagcc-3′ and reverse 5′-ccccccgtcgacgtcacgatgcggccgctcgagtcgg-3′ and by cloning it into pmCherry-N3. pGW1H-unROP18 ME49 and pGW1H-unROP18 RH-YFP containing the unprocessed forms of ROP18 were generated by PCR amplification from genomic DNA of ME49 and RH-YFP T. gondii strains using the following primers: forward 5′-ccccccgtcgaccaccatgttttcggtacagcggcc-3′ and reverse 5′-ccccccgtcgacttagtcaagtggatcctggttagtatggacctcttctgtgtggagatgttcctgc-3′ and subsequent cloning into the SalI site of pGW1H (British Biotech). The C-terminally Ty-tagged mature forms of ROP18 were amplified from pGW1H-unROP18 ME49 and pGW1H-unROP18 RH-YFP using the following primers: forward 5′-ccccccgtcgaccaccatggaaagggctcaacaccgggta-3′ and reverse 5′-ccccccgtcgacttagtcaagtggatcctggttagtatggacctcttctgtgtggagatgttcctgc-3′ and cloned into pGW1H by SalI digestion. Pfu-polymerase (Promega) was used for PCR amplification and primers were from Operon Biotechnologies GmbH. Restriction enzymes were from New England Biolabs. All constructs were verified by sequencing.
gs3T3 cells (Invitrogen), Mifepristone-inducible gs3T3-Irga6 cells (Hunn et al., 2008), A31 3T3 cells (ATCC, CCl-163), Atg5−/− and the corresponding wt control immortalized mouse fibroblasts (Kuma et al., 2004, kindly provided by Martin Krönke and Nobura Mizushima), MyD88−/− MEFs (Adachi et al., 1998, kindly provided by Manolis Pasparakis), Irga6−/− MEFs (Martens et al., 2005), L929 cells (ATCC CCl-1), HFF cells (ATCC, CRl-1634) and C57BL/6 MEFs were cultured in DMEM, high glucose (Invitrogen) supplemented with 10% fetal calf serum (FCS) (Biochrom), 2 mM l-glutamine, 1 mM sodium pyruvate, 1× MEM non-essential amino acids, 100 U ml−1 penicillin and 100 mg ml−1 streptomycin (all PAA). Transient transfection of mouse fibroblasts was conducted using FuGENE6 (Roche) according to the manufacturer's instructions. Cells were induced with 200 U ml−1 of mouse IFNγ (Peprotech) or 10−9M Mifepristone (Invitrogen) for 24 h.
To analyse the influence of other IRG proteins on the loading of Irga6 onto PVs of T. gondii strain ME49 pools of pGW1H-IRG expression constructs were transiently transfected into Mifepristone-induced gs3T3-Irga6 cells (Hunn et al., 2008) grown on coverslips in six-well plates. In all cases 400 ng of each construct were co-transfected in a total amount 2 µg of DNA. Empty vector was used to adjust DNA amounts if less than five constructs were transfected.
The following immunoreagents were used: rabbit anti-Irga6 antiserum 165/3 (Martens et al., 2004), mouse anti-Irga6 monoclonal antibodies (mAb) 10E7 and 10D7 (Papic et al., 2008), mouse anti-Irgm3 monoclonal antibody anti-IGTP (BD Biosciences, 610881), goat anti-Irgb6 antiserum A20 (Santa Cruz Biotechnology, sc-11079), rabbit anti-Irgb6 antiserum 141/1 was raised against recombinant bacterial full-length protein (N. Pawlowski, unpublished data), mouse anti-Irgb6 monoclonal antibody B34 (Carlow et al., 1998), rabbit anti-Irgm2 antiserum H53/3, raised against the N-terminal peptide of Irgm2 from C57BL/6 and unreactive against Irgm2 from 129 strain mice (Martens et al., 2005 and J.C. Howard, unpublished data), rabbit anti-Irgd antiserum 2078/3 (Martens et al., 2004), rabbit anti-Irgd antiserum 081/1 was raised against bacterially synthesized full-length protein (N. Pawlowski and G. Vopper, unpublished data), rabbit anti-Irgb10 antiserum (Coers et al., 2008), anti-Irgm1 antiserum L115 B0 (Martens et al., 2005), anti-T. gondii rabbit (BioGenex, PU125-UPE) and goat antisera (Abcam, ab23507), mouse IgG anti-GRA7 monoclonal antibody (Bonhomme et al., 1998) and mouse IgM anti-GRA7 monoclonal antibody TxE2 (Fischer et al., 1998), rabbit anti-ctag1 antiserum 2600 (Martens et al., 2005), rabbit anti-calnexin antiserum (StressGene, SPA-865), mouse anti-α-tubulin monoclonal antibody (Sigma-Aldrich, T 6074), mouse anti-Ty-tag monoclonal antibody (Bastin et al., 1996, kindly provided by Keith Gull), rat anti-LAMP1 monoclonal antibody (University of Iowa), anti-Akt (Cell Signaling, 9272) and anti-phosphoAkt (Cell Signaling, 9271) rabbit polyclonal antibodies, rabbit anti-PARP1 polyclonal antibody (Cell Signaling, 9542), Alexa 350/488/546/555/647-labelled donkey anti-mouse, rabbit and goat sera (Molecular Probes), donkey anti-rabbit- (GE Healthcare), donkey anti-goat- (Santa Cruz Biotechnology) and goat anti-mouse-HRP (horseradish peroxidase) (Pierce) antisera.
The serum 081/1, used to identify Irgd, produced occasional signals in IFNγ-stimulated Irgd−/− MEFs (S. Könen-Waisman, unpublished data). These signals were extremely faint compared with the strong signals from wt cells measured both by Western blot and immunofluorescence. Considering the significant homology between the IRG proteins we assume that the reagent is cross-reacting weakly on another family member. Nevertheless the counted frequency of positive vacuoles found with 081/1 corresponded with that seen with rabbit antiserum 2078/3 (Martens et al., 2004), a much weaker anti-peptide antiserum, used at high concentration.
To block PI3 kinase and G protein-coupled receptors overnight FCS-starved C57BL/6 MEFs were pretreated with wortmannin (0.5 µM), LY294002 (2-(4-morpholinyl)-8-phenyl-4H-1-benzopyran-4-one) (25 µM) and pertussis toxin (200 ng ml−1) for 6 h (all reagents were derived from Sigma-Aldrich and handled according to the manufacturers protocol). The extent of inhibition was tested by monitoring in Western blot the level of phospho-Akt (pAkt) after 10 min stimulation with EGF (epidermal growth factor) (100 ng ml−1) (Peprotech). To block caspase activity MEFs were pretreated with z-VAD-fmk (benzyloxycarbonyl-Val-Ala-Asp fluoromethyl ketone) pan-caspase inhibitor (100 µM) (Alexis Biochemicals, 260-020-M005) for 2 h, and the degree of blockade was analysed by monitoring the processing of PARP1 (poly-ADP ribose polymerase 1) 6 h after TNFα (40 ng ml−1) (Peprotech) plus cycloheximide (Chx) (10 µg ml−1) stimulation in Western blot. Inhibition of microtubule polymerization was achieved by incubating MEFs in 10 µM nocodazole in DMSO (Sigma-Aldrich) for 1 h and was monitored microscopically after performing immunostaining using anti-α-tubulin mouse monoclonal antibody.
To assay IRG protein association with the PV under conditions of blocked signalling pathways or inhibited microtubule polymerization, IFNγ-stimulated MEFs were pretreated as described above or left untreated as a control, then infected with ME49 T. gondii for 2 h and stained for Irgb6 (serum A20) and Irga6 (mAb 10D7). To study MyD88 involvement in PV loading by IRG proteins IFNγ-stimulated MyD88−/− and wt MEFs were infected with ME49 T. gondii and stained for Irgb6 (serum A20) and Irga6 (mAb 10D7).
The following T. gondii strains were used: type I virulent RH (Lecomte et al., 1992), RH-Δrop16 [in which the ROP16 locus has been deleted through double homologous recombination using HXGPRT for selection and PCR for confirmation of the deletion, as previously described (Saeij et al., 2008)], RH-YFP (Gubbels et al., 2003) and BK (Winsser et al., 1948); type II avirulent ME49 (Guo et al., 1997), NTE (Gross et al., 1991), avirulent recombinant T. gondii strains S22 (Saeij et al., 2006) and S22-LC37, the latter harbouring a cosmid containing four ROP5 genes (ROP5A–D) along with two adjacent genes (annotated gene models TGME49_108070 and TGME49_108060) from the RH strain and introduced using bleomycin selection; type III avirulent CTG strain (Pfefferkorn and Kasper, 1983, kindly provided by Dominique Soldati-Favre). Tachyzoites of different T. gondii strains were passaged in HS27 cells (Martens et al., 2005), and used for infection of untreated, transiently transfected, IFNγ- and/or Mifepristone-induced fibroblasts at a multiplicity of infection (moi) from 5 to 10 as described previously (Martens et al., 2005). Toxoplasma infection of MEFs was synchronized according to Kafsack et al. (2004; 2007;). In brief, the parasites were resuspended to 5 × 106 parasites per millilitre in invasion non-permissive Endo buffer (44.7 mM K2SO4, 10 mM MgSO4, 106 mM sucrose, 5 mM glucose, 20 mM Tris–H2SO4, 3.5 mg ml−1 BSA, pH 8.2). One millilitre of tachyzoite suspension was added to each well on the six-well plate, the plates centrifuged at 1500 r.p.m. for 2 min and then placed in the incubator. The infection was synchronized by replacing the Endo buffer by permissive medium (IMDM + 10 mM Hepes buffer, pH 7.4, and 5% FCS) for 2 min. Free parasites were subsequently removed by repeated washing with medium until no free parasites could be detected microscopically. At various times after infection, cells were washed with PBS and fixed in PBS/3% paraformaldehyde. Non-synchronized cells were handled throughout in IMDM/5% FCS, parasites were added at time zero, and the cells were examined at various times thereafter after washing and fixation.
The growth of T. gondii was analysed using the 3H-uracil incorporation assay (Pfefferkorn and Guyre, 1984). IFNγ-induced MEFs were infected with specified T. gondii strains for 24 h at moi 0.3, 1 and 3. The cultures were labelled with 0.3 µCi well−1 of 3H-uracil (3HU, Harmann Analytic) for 24 h and then frozen at −20°C. The amount of radioactivity incorporated into the proliferating parasites was determined in a β-scintillation spectrometer. The data are shown either as radioactive counts (Fig. S7), which are proportional to the parasite growth, or as the percentage of parasite growth inhibition caused by IFNγ treatment (Fig. 9C). Growth inhibition was defined as follows:
where system background is 3HU counts in an uninfected, non-induced culture.
Immunocytochemistry was performed on paraformaldehyde-fixed cells as described earlier (Martens et al., 2004; 2005;); the images were taken with an Axioplan II fluorescence microscope and AxioCam MRm camera and processed by Axiovision 4.7 (all Zeiss) and Image J softwares (http://rsb.info.nih.gov/ij/). 4′,6-Diamidine-2′-phenylindole dihydrochloride (DAPI, Invitrogen) was used for nuclear counterstaining at a final concentration of 0.5 µg ml−1. Intracellular parasites were identified by observing the vacuolar localization of the T. gondii protein GRA7 or by distinct pathogen appearance in phase contrast.
Live cell imaging was performed as described earlier (Zhao et al., 2009a).
The measurements were performed using the Image J (http://rsb.info.nih.gov/ij/) and Axiovision 4.7 (Zeiss) software. To measure the intensity of fluorescent signal on a labelled PVM, two lines were drawn at right angles across the long and short axes of the vacuole, and pixel intensity profiles obtained for each line (Fig. S1). The first and last values for each line provided four estimates of ‘background’ signal, while the four peaks where each line crossed the margins of the PVM gave four independent values for the signal strength at the vacuole. The signal intensity for the vacuole was given as the mean of the four peak values minus the mean of the four background values.
Cells were lysed in 1% Triton X-100/PBS/Complete Mini Protease Inhibitor Cocktail, EDTA-free (Roche) or 1× sample buffer (80 mM Tris-HCI, 5 mM EDTA, 34% Sucrose, 3.2% SDS, 40 mM DTT, bromophenol blue). Post-nuclear supernatants were subjected to SDS-PAGE and Western blot. Membranes were probed for IRG proteins with the indicated primary and HRP-coupled secondary antibodies for chemiluminescence.
For those experimental paradigms (Figs 6A and 8B), for which the number of experiments was large enough, significance was assessed with a modified Student's t-test after Dixon and Massey (Dixon and Massey, 1969). This t-test allows the comparison of sample sizes less than 30 and with unequal variances. For those experimental paradigms for which the number of experiments did not exceed n = 3 (Figs 5A and 8A), original data from the individual experiments were pooled and compared with a chi-squared test (Greenwood and Nikulin, 1996). Sample parameters were considered to be significantly different throughout this study with P < 0.05. The significances of differences between pixel intensity distributions shown in Figs 5B, 6F, 7 and 8D were estimated by the Mann–Whitney U-test (Mann and Whitney, 1947).
We would like to thank Michael L. Reese of Stanford University for valuable discussions during the preparation of the manuscript. We thank Rita Lange, Claudia Poschner, Natasa Papic, Matthias Müllenbeck and Ashiq Hussain for valuable technical support at various points during this study and Nikolaus Pawlowski for bacterially expressed, purified Irgb6 and Irgd proteins. We are extremely indebted to Ansgar Büschges, Sylvia Gruhn and Daniel Zivkovic for the time and trouble they took to assist with statistical analysis. We are grateful to the following scientists for the provision of specific reagents, acknowledged individually in the text: Dominique Soldati-Favre, Douglas Carlow, Keith Gull, Martin Krönke, Nobura Mizushima, Manolis Pasparakis and Jens Zerrahn. AK, JPH and DP were supported in part by the International Graduate School for Genetics and Functional Genomics and by the Graduate School for Biological Sciences of the University of Cologne. J.C. was supported by the Charles A. King Trust Postdoctoral Research Fellowship. This work was supported in part by the following grants to JCH from the Deutsche Forschungsgemeinschaft: SPP1110, Innate Immunity; SFB670, Cell Autonomous Immunity; SFB635 Post-translational Control of Protein Function; SFB680 Molecular Basis of Evolutionary Innovation. Support to JCB was through the NIH (AI21423 and AI73756). YCO was supported by a Smith Stanford Graduate Fellowship and the National Science Foundation. JPB was supported by the NIH (F32AI60636). MLR was supported by the American Cancer Society. [Correction added on 16 March 2010, after first online publication: acknowledgement of funding sources]
Additional Supporting Information may be found in the online version of this article:
Fig. S1. Analysis of IRG pixel intensity on T. gondii PVs.
Details of this analysis are given in Experimental procedures. To measure the intensity of IRG signal on T. gondii PVs two lines were drawn approximately at right angles across each vacuole (A). Each line thus crossed the ‘margin’ of the vacuole twice, giving a total of four values for each vacuole using the Image J and Axiovision 4.7 software. The pixel intensity of each vacuole was defined as the mean of these four values after background subtraction (B). To investigate how much variation in signal intensity measurements is caused by inhomogeneity of the IRG signal around the rim of the PV, 20 profiles were created by drawing 20 parallel lines through each of three more or less brightly Irgb6- positive vacuoles (stained by serum A20). The mean values of pixel intensity were calculated from each profile and presented as single dots and the arithmetic means are given as horizontal lines (C). Variation of Irgb6 intensity around the rim of single PVs clearly does not account for the total heterogeneity of IRG protein signal shown on Fig. 2A and B and elsewhere as the different signal intensities on the three vacuoles can be clearly distinguished. (D) Selected frames of two time-lapse videos of Irgb6- FLAG-EGFP loading on ME49 T. gondii PV. MEFs were transfected with the expression plasmid pEGFP-N3-Irgb6-FLAG and simultaneously induced with IFNγ. After 24 h, the cells were infected with T. gondii ME49 strain in microscope slide chambers as described in Zhao et al. (2009a) and monitored continuously in order to document the entry of individual parasites and the subsequent accumulation of Irgb6-FLAG-EGFP on the PV. Arrowheads indicate the location of the analysed T. gondii PVs.
Fig. S2. Inhibition of major signalling pathways and microtubule polymerization.
A. The blockade of PI3 kinase and G protein-coupled receptors was demonstrated by Western blot for phospho-Akt (pAkt). MEFs were treated with wortmannin (W), LY294002 (LY) or pertussis toxin (PT) for 6 h as described in Experimental procedures. Inhibited cells were stimulated by EGF for 10 min to induce Akt phosphorylation. Calnexin and total Akt served as a loading control. B. To inhibit caspases MEFs were treated with z-VAD-fmk for 2 h followed by stimulation with TNFα for 6 h in the presence of cycloheximide (Chx), as described in Experimental procedures. The amount of PARP1 processing by caspases was analysed by Western blot. Calnexin served as a loading control.
C. Inhibition of microtubule polymerization was monitored microscopically by immunostaining with an anti-α-tubulin mouse monoclonal antibody. MEFs were induced with IFNγ for 24 h and treated with nocodazole, or DMSO as control, for 1 h, as described in Experimental procedures. Treated cells were infected with T. gondii ME49 strain and loading of parasite PVs was monitored 2 h after infection by immunostaining for Irgb6 (serum A20).
Fig. S3. Irga6 aggregates do not colocalize with lysosomal marker LAMP1 in Atg5-/- fibroblasts. Cells were prepared as described in Fig. 5A and immunostained for Irga6 (mAb 10D7) and LAMP1 (mAb 1D4B). No obvious colocalization of Irga6 with LAMP1 in wt and Atg5-/- fibroblasts was observed. Arrows indicate intracellular parasites identified by phase contrast (PhC), and arrowheads indicate Irga6 aggregates.
Fig. S4. Frequencies of IRG protein-positive vacuoles detected by specific antibody reagents at different dilutions: saturation of frequency estimates. IFNγ-induced C57BL/6 MEFs were infected with T. gondii ME49 for 2 h. IRG proteins were detected by serial twofold dilution of antibody reagents around the dilutions typically used for experiments followed by an appropriate secondary reagent to estimate loaded vacuole frequencies. The experimental dilutions for each reagent were as follows: for Irgb6: mAb B34 at 1/1000 (3.4 mg ml-1 stock), serum A20 at 1/200; for Irgb10: serum anti-Irgb10 at 1/2000; for Irga6: mAb 10E7 at 1/1000 (3.7 mg ml-1 stock), mAb 10D7 at 1/2000 (4.3 mg ml-1 stock), serum 165/3 at 1/8000; for Irgd: serum 081/1 at 1/4000. The most concentrated dilution is designated as 1 (mAb B34 at 1:250, serum A20 at 1:50, serum anti-Irgb10 at 1:500, mAb 10E7 at 1:100, mAb 10D7 at 1:500, serum 165 at 1:2000, serum 081/1 at 1:4000). IRG-positive PVs were counted blind from 100–200 intracellular parasites. Frequency estimates for loaded vacuoles were independent of antibody or antiserum dilution in the range tested.
Fig. S5. Irga6-ctag1-EGFP loads before Irgd-ctag1-Cherry onto T. gondii ME49 strain PV. C57BL/6 MEFs were induced with IFNγ and transfected simultaneously with constructs expressing Irga6- ctag1-EGFP and Irgd-ctag1-Cherry. After 24 h, cells were infected with T. gondii ME49 strain in microscope slide chambers and observed by live cell imaging for the accumulation of IRG proteins. Successive 3 min frames from one vacuole (arrow) show Irga6 visibly loading several frames before Irgd.
Fig. S6. Irga6 and Irgb6 pixel intensity profiles of RH-YFP PVs in IFNγ-induced cells. IFNg-induced MEFs were infected with the T. gondii strain RH-YFP for 2 h. The pixel intensities of the Irga6 (mAb 10D7, red) and serum Irgb6 (A20, blue) signals at the RH-YFP (green) PVM across transects of the vacuole are displayed as a function of distance (μm). Five representative PVs of the three categories Irga6 and Irgb6 double-positive (A), Irga6 single-positive (B) and double-negative (C) are given (see also Fig. 8E). The baseline of the A20 serum staining is high due to diffuse background staining of the blue second stage reagent.
Fig. S7. IFNγ-restrained proliferation of T. gondii is not affected by the virulence-associated ROP proteins, ROP5 and ROP16. The growth of RH-Δrop16, S22-LC37 (carrying the cosmid expressing 4 ROP5 and 2 other genes) and control RH and S22 T. gondii strains was measured by 3H-uracil incorporation as described in Experimental procedures. The data are presented in radioactive counts per 3 min. Black, light grey and dark grey bars indicate proliferation of the parasite in MEFs untreated, stimulated with 10 U ml-1 and 100 U ml-1 of IFNγ respectively.
Table S1. Summary of experiments analysing the correlated loading of selected pairs of IRG proteins on to the ME49 PV.
Video S1. Time-lapse video of Irga6-ctag1-EGFP association with the T. gondii PV. IFNγ-treated MEFs were transfected with the construct expressing Irga6-ctag1-EGFP and infected with T. gondii ME49. Time-lapse video was started immediately after infection and the images were collected every 30 s (see also Fig. 2A). The video is presented at 6 frames per second.
Video S2. Time-lapse video of Irga6-ctag1-EGFP association with the T. gondii PV. IFNγ-treated MEFs were transfected with the construct expressing Irga6-ctag1-EGFP and infected with T. gondii ME49. Time-lapse video was started 1 h after infection and the images were collected every 3 min (see also Fig. 2B). The video is presented at two frames per second. Out of focus frames were excluded from the movie.
Please note: Wiley-Blackwell are not responsible for the content or functionality of any supporting materials supplied by the authors. Any queries (other than missing material) should be directed to the corresponding author for the article.