PMCCPMCCPMCC

Search tips
Search criteria 

Advanced

 
Logo of jexpmedHomeThe Rockefeller University PressThis articleEditorsContactInstructions for AuthorsThis issue
 
J Exp Med. 2010 April 12; 207(4): 807–821.
PMCID: PMC2856038

Human cytomegalovirus elicits fetal γδ T cell responses in utero

Abstract

The fetus and infant are highly susceptible to viral infections. Several viruses, including human cytomegalovirus (CMV), cause more severe disease in early life compared with later life. It is generally accepted that this is a result of the immaturity of the immune system. γδ T cells are unconventional T cells that can react rapidly upon activation and show major histocompatibility complex–unrestricted activity. We show that upon CMV infection in utero, fetal γδ T cells expand and become differentiated. The expansion was restricted to Vγ9-negative γδ T cells, irrespective of their Vδ chain expression. Differentiated γδ T cells expressed high levels of IFN-γ, transcription factors T-bet and eomes, natural killer receptors, and cytotoxic mediators. CMV infection induced a striking enrichment of a public Vγ8Vδ1-TCR, containing the germline-encoded complementary-determining-region-3 (CDR3) δ1–CALGELGDDKLIF/CDR3γ8–CATWDTTGWFKIF. Public Vγ8Vδ1-TCR–expressing cell clones produced IFN-γ upon coincubation with CMV-infected target cells in a TCR/CD3-dependent manner and showed antiviral activity. Differentiated γδ T cells and public Vγ8Vδ1-TCR were detected as early as after 21 wk of gestation. Our results indicate that functional fetal γδ T cell responses can be generated during development in utero and suggest that this T cell subset could participate in antiviral defense in early life.

The fetus and young infant have a high susceptibility to infections with intracellular pathogens, suggesting that T cell–mediated immune responses are different in early life. A number of viruses, including human CMV, herpes simplex type 2, respiratory syncytial virus, and HIV, cause more severe or rapidly progressive disease in early life as compared with later life (Stagno, 2001; Marchant and Goldman, 2005). It is generally accepted that this increased susceptibility to viral infections is related to the immaturity of the neonatal immune system. This includes intrinsic defects of conventional T cells, especially CD4 αβ T cells, and impaired DC responses (Lewis and Wilson, 2001; White et al., 2002; Maródi, 2006; Levy, 2007; Lee et al., 2008). CMV is the most common cause of congenital infection, affecting 0.2% of all live births in industrialized countries and up to 3% in developing countries (Stagno, 2001). Although CMV infection causes no detectable symptoms in immunocompetent adults, ~20% of newborns with congenital infection develop serious symptoms, including cerebral malformations, multiple organ failure, deafness, and mental retardation (Stagno, 2001; Dollard et al., 2007).

γδ T cells are T cells expressing γ and δ chains as a TCR on their cell surface instead of α and β chains as in conventional CD4 and CD8 αβ T cells. Together with αβ T cells, they have been conserved for >450 million years of evolution (Hayday, 2000). γδ T cells are the prototype of unconventional T cells; they can react rapidly upon activation and show MHC-unrestricted activity (Hayday, 2000; Holtmeier and Kabelitz, 2005). Thus, they are not influenced by MHC down-regulation strategies used by viruses such as CMV to escape conventional T cells (Wilkinson et al., 2008). Studies in several species have shown an important role for γδ T cells in protection against infection, in tumor surveillance, in immunoregulation, and in tissue repair (Hayday, 2000; Wang et al., 2001; Holtmeier and Kabelitz, 2005; Pennington et al., 2005; Toulon et al., 2009). In general, they show a rapid and robust response before the development of the adaptive immunity mediated by conventional T cells. In comparison with αβ T cells, γδ T cells are not abundant in the peripheral blood but are highly enriched in tissues like the gut epithelium (Hayday, 2000; Holtmeier and Kabelitz, 2005). The majority of γδ T cells in human adult peripheral blood use the TCR V region pair Vγ9Vδ2 (note that according to an alternative nomenclature the Vγ9 chain is also termed Vγ2 [Holtmeier and Kabelitz, 2005]). This subset has been shown to react specifically toward nonpeptide low molecular weight phosphorylated metabolites (so-called phosphoantigens) and has been the subject of several clinical trials (Wilhelm et al., 2003; Dieli et al., 2007; Kabelitz et al., 2007).

Probably in all species, γδ T cells are the first T cells to develop (Hayday, 2000). In contrast to adult peripheral blood γδ T cells, human neonatal cord blood γδ T cells express diverse Vγ and Vδ chains paired in a variety of combinations (Morita et al., 1994). Thus the adult-like Vγ9Vδ2 subpopulation only represents a small fraction of the neonatal γδ T cells (Parker et al., 1990; Morita et al., 1994; Cairo et al., 2008). Further illustrating the differences between adult and neonatal γδ T cells, is the demonstration that in vitro exposure toward the same pathogen (Escherichia coli or Pseudomonas aeruginosa) results in expansion of Vδ2+ γδ T cells in adult peripheral blood but of Vδ1+ γδ T cells in cord blood (Kersten et al., 1996). In mice, γδ T cells are important for the protection against an intestinal parasite infection in early life but not in adult life (Ramsburg et al., 2003), and during human T cell ontogeny γδ T cells mature before αβ T cells (De Rosa et al., 2004). However, so far it is not known whether pathogens in early life can activate human γδ T cells. To gain insight into the ability of γδ T cells to mount responses to viruses during fetal life, we studied the changes occurring in the γδ T cell compartment during congenital CMV infection.

RESULTS

CMV infection in utero induces expansion of fetal γδ T cells in newborns

To address whether human fetal γδ T cells are responsive to CMV infection in utero, we first compared the percentage of γδ T cells among all T cells in cord blood samples derived from 19 CMV-infected newborns versus 22 control CMV-uninfected newborns. In CMV-infected newborns, the percentage of γδ T cells was significantly higher than in CMV-uninfected newborns (Fig. 1 A). To exclude the possibility that this higher percentage of γδ T cells was the result of a decreased number of αβ T cells, we determined the absolute number of γδ T cells per microliter of blood. Indeed, significantly more γδ T cells were present per microliter of cord blood in CMV-infected newborns in comparison with controls (Fig. 1 B). The higher number of γδ T cells correlated with a higher percentage of γδ T cells expressing the proliferation marker Ki-67 in CMV-infected newborns (Fig. 1 C).

Figure 1.
CMV infection in utero induces an expansion of γδ T cells in newborns. (A) Percentage of γδ T cells of total T cells (CMV+, n = 19; CMV, n = 22). (B) Absolute number of γδ T cells per microliter ...

The expansion of γδ T cells in CMV-infected newborns is restricted to Vγ9 cells, irrespective of the usage of the Vδ chain

To further define specific subsets of γδ T cells in cord blood of CMV-infected newborns, flow cytometry analysis was performed with antibodies specific against Vγ9, Vδ1, Vδ2, and Vδ3. In combination with the pan-γδ TCR antibody, the Vγ9 antibody can make distinction between Vγ9+ and Vγ9 γδ T cells (Fig. 2 A). Vγ9 is the only member of the VγII family; thus the Vγ9 cells express Vγ chains of the VγI family (Hayday, 2000). The combination of Vδ1, Vδ2, and Vδ3 antibodies stained the vast majority (~90%; unpublished data) of the cord blood γδ T cells. This approach allows us to identify six γδ T cell subpopulations in cord blood: Vγ9+Vδ1+, Vγ9Vδ1+, Vγ9+Vδ2+, Vγ9Vδ2+, Vγ9+Vδ3+, and Vγ9Vδ3+. We detected higher percentages of γδ T cells negative for Vγ9, including Vγ9Vδ1+, Vγ9Vδ2+, and Vγ9Vδ3+ γδ T cells in CMV-infected newborns compared with uninfected newborns (Fig. 2, A and B). On a selected number of CMV-uninfected and CMV-infected newborns, we performed a more detailed analysis of the γ chain usage. In CMV-uninfected newborns, there was a slight preference for Vγ4 and Vγ9, whereas upon CMV infection the VγI family members Vγ4 and Vγ8 were highly expanded (Fig. S1).

Figure 2.
The expansion of γδ T cells in CMV-infected newborns is restricted to Vγ9 γδ T cells, irrespective of the usage of the Vδ chain. (A) Expression of Vγ9 versus Vδ1, Vδ2, or ...

γδ T cells from CMV-infected newborns are activated and differentiated

Next, we evaluated whether the expansion of fetal γδ T cells after congenital CMV infection was accompanied by activation and/or differentiation of these cells. A significant proportion of γδ T cells from CMV-infected newborns expressed the activation marker HLA-DR, whereas expression was virtually absent in uninfected controls (Table I). Down-regulation of CD27 and CD28 expression has been shown to be associated with advanced or late differentiation in CD8 αβ T cells upon CMV infection (Appay et al., 2002; Marchant et al., 2003; van Leeuwen et al., 2006). These markers have also been used to identify differentiated human γδ T cells (Morita et al., 2007). Although CD27CD28 γδ T cells were absent from CMV-uninfected newborns, a large proportion of γδ T cells showed this phenotype in CMV-infected newborns (Table I). This differentiation was most pronounced in the Vγ9 γδ T cell subpopulation (unpublished data). Collectively, these data clearly show that upon congenital CMV infection, γδ T cells are activated, undergo cell division, and become differentiated.

Table I.
Percentage of activation (HLA-DR) and differentiation (CD27, CD28) markers, NKRs (CD94, NKG2A, NKG2C, CD158, NKG2D, and KLRG1), cytotoxic mediators (perforin and granzyme A), and chemokine receptor CX3CR1 on γδ T cells derived from CMV-infected ...

Expression of NK receptors (NKRs), cytotoxic mediators, and IFN-γ is highly increased in γδ T cells of CMV-infected newborns

To gain insight into the function of fetal γδ T cells in newborns with congenital CMV infection, we compared the gene expression profiles of γδ T cells derived from three CMV-infected newborns versus three CMV-uninfected newborns. 1,622 genes were increased and 654 decreased upon infection (using the selection criteria described in Materials and methods; M > 0.05, P < 0.05). More than 100 genes associated with cell cycle showed increased expression upon CMV infection (as analyzed with DAVID; not depicted), coinciding with the expansion data (Fig. 1).

NKRs.

Expression of a range of NKR genes was increased in γδ T cells from CMV-infected newborns in comparison with γδ T cells from CMV-uninfected newborns (Fig. 3, KIR2DL1; Table S1). This included both activating and inhibitory receptors (Table S1) and involved all the NKR families: the killer immunoglobulin receptor (KIR) family, the C-type lectin family (CD94/NKG2A/NKG2C), and the natural cytotoxicity receptor (NCR) family (NKp46; Lanier, 2008). In CMV-uninfected newborns, there were either no or very few γδ T cells (CD94/NKG2A/NKG2C, CD158a/h [KIR2DL1/KIR2DS1], and CD158b/j [KIR2DL2/KIR2DS2]) or a significant fraction of γδ T cells (NKG2D and KLRG1) expressing NKR on their membrane, as determined by flow cytometry (Table I). In CMV-infected newborns, significantly more γδ T cells expressed all these NKRs (Table I).

Figure 3.
Gene expression analysis of γδ T cells derived from three CMV-infected newborns versus γδ T cells derived from three CMV-uninfected newborns. MA plot of differentially expressed genes in γδ T cells upon ...

Cytotoxic mediators.

In general, cytotoxic lymphocytes can kill target cells by two main mechanisms: exocytosis of granule-associated molecules, such as granzymes, perforin, and granulysin, or binding to receptors with ligands of the TNF superfamily (e.g., FasL and TRAIL). Among the >47,000 transcripts analyzed, the two genes displaying the most increased expression upon CMV infection were members of the granzyme family: granzyme B and granzyme H (Fig. 3). In addition, other granzyme family members (granzyme A and granzyme M), perforin, granulysin, FasL, and TRAIL were increased (Table S1). In CMV-uninfected newborns, there was either no or only a low percentage of γδ T cells expressing perforin and granzyme A, as demonstrated by flow cytometry (Table I). In CMV-infected newborns, the percentages of γδ T cells expressing perforin or granzyme A were highly increased (Table I). This expression was clearly associated with the late differentiation status of the γδ T cells (Fig. S2 A).

Chemokines and chemokine receptors.

The genes for the chemokines CCL3 (MIP-1α), CCL4 (MIP-1β), and CCL5 (RANTES), all ligands for CCR5, and two chemokine receptor genes (CCR5 and CX3CR1) showed increased expression in γδ T cells from CMV-infected newborns in comparison with γδ T cells from CMV-uninfected newborns (Table S1). CCR7 gene expression was decreased upon CMV infection (M = −2.27, A = 8.07, P = 0.03). In CMV-uninfected newborns, there were no or only a low percentage of γδ T cells expressing CX3CR1 (fractalkine receptor) on their membrane, as determined by flow cytometry (Table I). In CMV-infected newborns, the percentage of γδ T cells expressing CX3CR1 was highly increased (Table I), which was clearly associated with the late differentiation phenotype of the γδ T cells (Fig. S2 B).

Cytokines.

Only a limited number of cytokine genes showed increased expression in γδ T cells derived from CMV-infected newborns in comparison with γδ T cells derived from CMV-uninfected newborns (Table S1). IFN-γ was one of the most increased expressed genes (Fig. 3 and Table S1). Strikingly, gene expression of transcription factors known to be implicated in IFN-γ production, namely T-bet (M = 2.37, A = 6.64, P = 0.000112) and eomes (M = 3.02, A = 6.31, P = 0.000246), was highly increased. The high expression of T-bet was confirmed at protein level by flow cytometry in γδ T cells from CMV-infected newborns and was associated with the differentiation status of γδ T cells (Fig. 4 A). Almost all CD27CD28 γδ T cells expressed T-bet, whereas CD27+CD28+ γδ T cells expressed significantly lower levels of this transcription factor (median within CD27CD28 γδ T cells, 97%; median within CD27+CD28+ γδ T cells, 28%; P = 0.0006). In addition, T-bet expression per cell, as measured by the mean fluorescence intensity (MFI), was consistently much higher in CD27CD28 γδ T cells than in CD27+CD28+ γδ T cells (median within CD27CD28 γδ T cells, 318 MFI; median within CD27+CD28+ γδ T cells, 102 MFI; P = 0.0023). Upon a brief polyclonal stimulation in vitro, the majority of CD27CD28 differentiated γδ T cells of CMV-infected newborns produced IFN-γ (Fig. 4 B), whereas the CD27+CD28+ γδ T cells produced significantly less IFN-γ (median within CD27CD28 γδ T cells, 68%; median within CD27+CD28+ γδ T cells, 22%; P = 0.0006). T-bet and IFN-γ expression within γδ T cells from CMV-uninfected newborns were similar to the expression found within CD27+CD28+ γδ T cells from CMV-infected newborns (unpublished data).

Figure 4.
Differentiated (CD27CD28) γδ T cells from CMV-infected newborns express highly the transcription factor T-bet and produce high levels of IFN-γ. Flow cytometry plots for T-bet (A) and IFN-γ (B), gated on ...

The CDR3δ1 and CDR3δ2 are highly restricted upon congenital CMV infection

To study the impact of CMV infection during fetal life on the TCR repertoire of γδ T cells, we assessed the degree of junctional diversity of the complementary-determining-region-3 (CDR3) of the Vδ1 (CDR3δ1) and Vδ2 (CDR3δ2) chains by spectratyping on 11 CMV-uninfected and 13 CMV-infected cord blood samples. CMV-uninfected cord blood samples showed polyclonal profiles for both CDR3δ1 (as described previously; Beldjord et al., 1993) and CDR3δ2. In contrast, the CDR3δ1 and CDR3δ2 repertoires became highly restricted in the vast majority of CMV-infected newborns (Fig. 5 A and Fig. S3). To quantify this restriction, we calculated an index of oligoclonality for CDR3δ1 and CDR3δ2 as described previously (Déchanet et al., 1999; Pitard et al., 2008). For both CDR3s, the index of oligoclonality was significantly higher in CMV-infected newborns than in CMV-uninfected newborns (Fig. 5 B). Moreover, the restriction of CDR3δ1 of CMV-infected newborns was enriched for the same length (11 aa) in all CMV-positive newborns (Fig. 5 A, arrows). This length was either absent or minimally present in CMV-uninfected newborns (Fig. 5 A). In contrast to CDR3δ1, the length of the enriched CDR3δ2 sequences in CMV-infected newborns varied from newborn to newborn (Fig. S3). It is of note that CMV-infected newborn Pos10 showed a polyclonal CDR3δ1 repertoire corresponding with the absence of CD27CD28 differentiated Vδ1+ γδ T cells (Fig. 5 A). In contrast, Vδ2+ γδ T cells of this newborn were well differentiated, corresponding to a restricted CDR3δ2 repertoire (Fig. S3).

Figure 5.
The CDR3δ1 and CDR3δ2 repertoire of γδ T cells from CMV-infected newborns are oligoclonal, and CDR3δ1 is highly enriched for a single sequence. (A) Spectratyping plots of the CDR3δ1 of CMV-uninfected and ...

Public germline-encoded CDR3δ1 and CDR3γ8 sequences are highly enriched in CMV-infected newborns

Because the CDR3δ1 of CMV-infected newborns was highly enriched at 11 aa, we wondered whether this region included the same or similar sequences. Strikingly, at amino acid level in all 12 sequenced CMV-infected newborns the CDR3δ1 of 11 aa had exactly the same sequence: CALGELGDDKLIF, or ELGDD for short (Table S2; Fig. 5 A). At the nucleotide level, two variants were observed: the first D of ELGDD was either formed by the ga of the diversity gene δ3 (Dδ3) and the c of the joining gene δ1 (Jδ1) or completely formed by the gat of the Dδ3 (Table S2, dark gray). Besides ELGDD itself, few longer variants were present in some CMV-infected newborns, which were enriched as well, containing one (Pos3) or two (Pos3 and Pos11) extra Ts after the first D of ELGDD (Table S2). In contrast to the other CDR3δ1 sequences, the highly enriched ELGDD sequence did not contain P/N additions and was thus completely germline encoded (Table S2).

In comparison with CDR3δ1, the degree of shared CDR3δ2 sequences among the CMV-infected newborns was much less clear (Table S3). Among eight CMV-infected newborns, three exhibited enrichment of the same CDR3δ2 sequence (Pos8, Pos9, and Pos10; Table S3). No other obvious similarities were found between different enriched CDR3δ2 sequences of different CMV-infected newborns. Vδ1 almost always paired with Jδ1, whereas Vδ2 had a preference for Jδ3 (Table S2 and Table S3). Sequencing of CDR3δ1 and CDR3δ2 of CMV-uninfected newborns confirmed the polyclonal repertoire as found by spectratyping (Table S2 and Table S3).

We wondered whether the Vδ1 chain, containing the public CDR3δ1, from CMV-infected newborns cells had a preference for pairing with specific Vγ chains. By costaining of Vδ1 and Vγ2/3/4, Vγ5/3, Vγ8, or Vγ9, we determined that within CMV-uninfected newborns Vδ1 had a preference for pairing with Vγ2/3/4 (Fig. 6 A), whereas Vδ2 and Vδ3 had rather a preference for Vγ9 and Vγ5/3, respectively (not depicted). In contrast, in CMV-infected newborns with highly expanded γδ T cells, Vδ1 had a clear preference for pairing with Vγ8 (Fig. 6 A), whereas Vδ2 and Vδ3 had rather a preference for Vγ2/3/4 (not depicted). Because of this preferential pairing of Vδ1 with Vγ8, we performed spectratyping for CDR3γ8 on six CMV-uninfected and six CMV-infected newborns. The CDR3γ8 of CMV-uninfected newborns showed a polyclonal repertoire. In contrast, the CDR3γ8 repertoire became highly restricted in CMV-infected newborns, showing a high enrichment at a length of 11 aa in five out of six CMV-infected newborns. The sixth CMV-infected newborn (Pos13) had a high enrichment at 12 aa (Fig. 6 B). Sequencing revealed that the CDR3γ8 sequences at 11 aa contained all the same sequence: CATWDTTGWFKIF (DTTGW for short). Pos13 had an extra Y after D (Fig. 6 B; Table S4). This sequence was not detected in CMV-uninfected newborns (Table S4). As for the public CDR3δ1 sequence, the public CDR3γ8 was completely germline encoded (Table S4).

Figure 6.
The Vδ1 chain on γδ T cells of CMV-infected newborns preferentially pairs with a public Vγ8 chain. (A) The percentage of Vδ1+ γδ T cells positive for Vγ2/3/4, Vγ5/3, Vγ8, ...

The public Vγ8Vδ1 TCR reacts against CMV-infected target cells

To verify whether the public Vγ8Vδ1 TCR reacts against CMV-infected target cells, we generated γδ T cell clones expressing the public TCR containing the CDR3δ1-ELGDD and CDR3γ8-DTTGW from CMV-infected newborns Pos4 (11 public clones) and Pos6 (21 public clones). All clones expressing CDR3δ1-ELGDD coexpressed CDR3γ8-DTTGW, whereas clones with a different CDR3δ1 expressed other CDR3γ’s (unpublished data), showing in a direct way the preferential pairing between CDR3δ1-ELGDD and CDR3γ8-DTTGW. A brief coincubation (6 h) of public clones with CMV-infected human embryonic lung fibroblasts induced IFN-γ production, which was blocked by the presence of a soluble anti-CD3 antibody (OKT3) showing the involvement of the public Vγ8Vδ1 TCR/CD3 complex in the recognition of CMV-infected target cells (Fig. 7 and Fig. S4). Control γδ T cell clones of CMV-uninfected newborns did not show CMV-induced IFN-γ production. To gain insight into the antiviral activity of the γδ T cell clones, we conducted additional experiments. Public clones killed infected target cells (Fig. 8 A) and inhibited CMV replication (between one and two log10 inhibition; Fig. 8 B), whereas control Vγ9Vδ2 T clones had no or only a moderate effect (Fig. 8).

Figure 7.
γδ T cell clones expressing the public Vγ8Vδ1 TCR display reactivity against CMV-infected cells via TCR/CD3. Clones were coincubated for 6 h with human embryonic fibroblasts not infected (white bars) or infected (gray bars) ...
Figure 8.
Public Vγ8Vδ1 clones kill CMV-infected target cells and inhibit CMV replication in vitro. (A) CMV-infected (TB40/E) human embryonic fibroblasts were coincubated with either γδ T cell clones expressing the public Vγ8Vδ1 ...

Differentiation and oligoclonal expansion of fetal γδ T cells can occur early during gestation

To explore the possibility that γδ T cells could develop a response toward CMV infection early during fetal life, we analyzed the γδ T cells from fetal cord blood samples collected between 20 and 29 wk of gestation (from 12 CMV-negative and 13 CMV-positive fetuses). At these earlier gestation times, the γδ T cells were already clearly differentiated (down-regulation of CD27 and CD28) and showed high expression of perforin (Fig. 9 A), granzyme A, and NKR (not depicted). From four CMV-infected fetuses, we performed spectratyping and sequencing for CDR3δ1 at time of delivery and at earlier gestation time (Fig. 9 B). We found that the CDR3δ1-ELGDD sequence was already enriched at as early as 21 wk of gestation (Fig. 9 B and Table S2). Few other CDR3δ1 sequences that were present at early gestation time were also present at time of delivery (Table S2, fetus Pos4 [14 aa] and fetus Pos13 [17 aa]). As observed at time of delivery, CDR3δ2 spectratyping showed more variability between fetuses (unpublished data). Furthermore, CDR3δ2 appeared to vary with time within the same fetus (Table S3, compare CDR3δ2 sequencing data of Pos4 at 20 wk, 5 d and at 40 wk, 0 d of gestation). Thus, the enriched CDR3δ1-ELGDD sequence appeared early during gestation in CMV-infected fetuses and remained present with time. In contrast, the enriched sequences of the CDR3δ2 were variable from one fetus to the other and changed during gestation time. Furthermore, the CDR3γ sequence associated with the CDR3δ1-ELGDD sequence, namely CDR3γ8-DTTGW, was also already enriched at as early as 21 wk of gestation (Table S4; CMV-infected newborn Pos4). Thus, despite the recent description of selective impairments of γδ T cells in preterm infants (Gibbons et al., 2009), γδ T cell are able to develop robust responses toward CMV infection in utero at as early as 21 wk of gestation.

Figure 9.
Differentiation and oligoclonal (CALGELGDDKLIF) expansion of fetal γδ T cells can occur early during gestation. (A) Expression of CD27/CD28 and perforin by γδ T cells from a representative CMV-uninfected (bottom) and a ...

DISCUSSION

In this study, we demonstrate that CMV infection in utero leads to the oligoclonal expansion and differentiation of fetal γδ T cells, which express high levels of NKR and cytotoxic mediators and produce IFN-γ. Both activating (e.g., activating KIR, NKG2C, and NKG2D) and inhibitory (e.g., inhibitory KIR, NKG2A, and KLRG1) NKRs were highly expressed in γδ T cells derived from congenitally infected newborns. This would allow them to sense CMV-induced changes in infected target cells; HLA-E (ligand for NKG2A/NKG2C) expression is increased upon CMV infection, whereas classical MHC class I (ligands for KIR) expression is decreased (Wilkinson et al., 2008). In comparison with conventional T cells, it has been described that adult γδ T cells express high levels of NKR, like members of the C-type lectin and the KIR family (Battistini et al., 1997; De Libero, 1999; Pennington et al., 2005). We confirmed the expression of KLRG1 on γδ T cells in CMV-uninfected newborns (Eberl et al., 2005) and also showed that NKG2D is constitutively expressed. In contrast, unlike NK cells (Dalle et al., 2005), other NKRs (CD94/NKG2x and KIR family members) were not expressed or were expressed at very low levels on γδ T cells from CMV-uninfected newborns. Thus the majority of NKR expression on adult γδ T cells is likely to be the consequence of infections after birth. CMV infection in utero induced the up-regulation of various cytotoxic mediators in fetal γδ T cells, including almost all members of the granzyme family, perforin, granulysin, FasL, and TRAIL. Perforin and granulysin are membrane-disrupting molecules and most granzymes have been shown to be involved in killing of target cells, with most evidence for granzyme B (Lieberman, 2003; Chowdhury and Lieberman, 2008). In addition, other granzyme-mediated antiviral mechanisms have been recently described: granzyme A plays a proinflammatory role (Metkar et al., 2008), granzyme M targets α-tubulin (Bovenschen et al., 2008), and granzyme H cleaves La, a phosphoprotein involved in cellular and viral RNA metabolism (Romero et al., 2009). It is of note that granzyme H cleaves an adenovirus-encoded granzyme B inhibitor (Andrade et al., 2007). Analysis of the profile of cytokine genes expressed in fetal γδ T cells derived from CMV-infected newborns revealed the restricted high expression of IFN-γ. In parallel, we detected elevated levels of the T-box transcription factors T-bet and eomes, which are involved in the rapid and vigorous IFN-γ production by γδ T cells (Yin et al., 2002; Chen et al., 2007). In contrast, expression of other transcription factor genes like GATA3 (Th2) or ROR-γt (Th17) was not affected, coinciding with the absence of modulation of cytokine genes associated with these Th subsets. Only two chemokine receptors were significantly increased in the microarray analysis: CCR5 and CX3CR1 (fractalkine receptor). Fractalkine can be produced by endothelial cells in the context of CMV infection (Bolovan-Fritts et al., 2004), thus possibly attracting differentiated CX3CR1+ fetal γδ T cells to the site of infection. Together, our data indicate that fetal γδ T cells generated in utero during CMV infection are equipped with a range of antiviral effector mechanisms, including IFN-γ production and granule-mediated cytotoxicity. Indeed, γδ T cell clones generated from CMV-infected newborns killed CMV-infected cells and limited CMV replication in vitro. It is therefore likely that they participate in the limitation of the viral spread in the fetus. In kidney-transplanted patients with acute CMV infection, expansion of γδ T cells is associated with the clinical resolution, suggesting a protective role of the expanded γδ T cells (Lafarge et al., 2001; Halary et al., 2005).

We demonstrated that CMV infection during fetal life leads to the oligoclonal expansion of γδ T cells, which is characterized by highly restricted CDR3δ1 and CDR3δ2 repertoires and by the high enrichment of a public CDR3δ1-CDR3γ8 sequence. Expanded γδ T cells were negative for Vγ9 and included Vδ1+, Vδ2+, and Vδ3+ cells. In contrast, in adult CMV-infected kidney transplanted patients, expanded γδ T cells do not include Vδ2+ cells and there is no restriction of CDR3δ2 (Déchanet et al., 1999). Vγ9Vδ2+ γδ T cells are very rare in the adult (Morita et al., 1994), providing a possible explanation of why Déchanet et al. (1999) did not detect any expansion of this subset in adults (Pitard et al., 2008).

TCR-δ chains have the highest potential diversity in the CDR3 loop (~1016 combinations) among all antigen receptor chains (TCR-α, TCR-β, TCR-γ, TCR-δ, IgH, and IgL) because multiple D gene segments can join together, all D gene segments can be read in all three open reading frames, and N nucleotides can be inserted into the junctions of each of the joining segments (Chien and Konigshofer, 2007). Therefore, it was surprising to identify a high enrichment of exactly the same CDR3δ1 sequence (i.e., public CDR3) in all fetuses with differentiated Vδ1+ γδ T cells upon congenital CMV infection (ELGDD). It has been suggested that much of the diversity of the CDR3 junctions of the δ chain may confer different affinities of the γδ TCR rather than the ability to recognize different ligands (Chien and Konigshofer, 2007). In addition, in adult CD8 αβ T cells, public CMV-reactive TCR sequences bind the MHC–peptide complexes with higher affinity than private MHC peptide–specific TCR sequences (Trautmann et al., 2005; Day et al., 2007). This suggests that the public CDR3δ1-ELGDD is enriched by recognition of a CMV-induced ligand with high affinity. Our results show for the first time, to our knowledge, the expansion of a public γδ TCR CDR3 in the context of an infection. Furthermore, we demonstrated that the public CDR3δ1 pairs with a public CDR3γ8 sequence (DTTGW), indicating that both the γ and δ chain are important for the recognition of the putative ligand. In addition, this public Vγ8Vδ1 TCR showed reactivity against CMV-infected target cells in vitro. It is of note that both the CDR3δ1-ELGDD and CDR3γ8-DTTGW were germline encoded, as the CDR3δ1 was only formed by the Vδ1 gene, one Dδ gene (Dδ3) and the Jδ1 gene, and the CDR3γ8 by the Vγ8 gene and the JγP1 gene, without any addition of P/N nucleotides. Similarly, the mouse T22/T10-binding CDR3δ does not contain N nucleotides (Adams et al., 2005; Chien and Konigshofer, 2007). This contrasts highly with αβ T cells, where the most critical amino acids in the CDR3α and CDR3β involved in the recognition of the MHC–peptide complex are encoded either completely or partially by N nucleotides (Davis et al., 1998; Chien and Konigshofer, 2007).

Despite the immaturity of the neonatal immune system and possible mechanisms of immunosuppression by regulatory T cells (Mold et al., 2008), CMV infection is efficient in stimulating vigorous responses of both γδ T cells and CD8 αβ T cells (Marchant et al., 2003) during fetal life. Studies in mice show that the protective role of γδ T cells in early life is not dependent on αβ T cells (Ramsburg et al., 2003). Conversely, in a model of West Nile virus infection, it has been shown that γδ T cells facilitate the CD8 αβ T cell response (Wang et al., 2006). In comparison with adult DC, fetal DC shows impaired functions (Goriely et al., 2004; Levy, 2007). Because γδ T cell differentiation is not dependent or is less dependent on DC in comparison with αβ T cells, it is reasonable to believe that fetal DC defects would not prevent γδ T cell differentiation upon fetal exposure to CMV. Instead, γδ T cells may recognize their ligands directly on infected cells in tissues (Hayday, 2009). Such activated fetal γδ T cells could, in turn, induce fetal DC maturation (Ismaili et al., 2002; Conti et al., 2005; Caccamo et al., 2006; Devilder et al., 2006; Eberl et al., 2009) and/or directly activate naive CD8 αβ T cells via antigen cross-presentation (Brandes et al., 2009), as shown in adult cells. Such mechanisms could contribute to the development of functional CD8 αβ T cell responses to CMV infection during fetal life (Marchant et al., 2003).

We conclude that human γδ T cells can mount a vigorous response to CMV infection during development in utero, providing an important mechanism by which the fetus can fight pathogens. Identification of the γδ TCR ligands induced upon CMV infection, like the putative ligand of the public Vγ8Vδ1 TCR, will likely be useful to design novel vaccination strategies against viral infection in early life.

MATERIALS AND METHODS

Study population.

This study was approved by the Hôpital Erasme and Hôpital Saint-Pierre ethical committees. Women with suspected primary CMV infection were referred to the Fetal Medicine Units of the Hôpital Erasme or Hôpital Saint-Pierre. Diagnosis of primary maternal infection was based on anti-CMV IgG seroconversion or on the detection of high titers of anti-CMV–specific IgM, as described previously (Liesnard et al., 2000). After maternal informed consent, 20–50 ml of cord blood was collected at birth (full term, >37 wk gestation). In some cases, fetal cord blood was collected at earlier gestation ages (~1 ml by cordocentesis). Diagnosis of congenital infection was based on the detection of CMV genome by PCR and/or by viral culture on amniotic fluid and/or on newborn urine collected during the first week of life. The study included 19 CMV-infected newborns and 22 uninfected control newborns as well as 13 infected and 12 uninfected fetuses. Symptomatic congenital infection was diagnosed in fetus Pos12 who had brain lesions at antenatal magnetic resonance imaging and an abnormal postnatal neurological development and in fetus Pos5 who had an abnormal postnatal neurological development.

Flow cytometry.

The following antibodies were used: CD3–pacific blue (clone SP34-2), γδ-PE (11F2), γδ-FITC (11F2), CD27-APC (L128), CD27-FITC (L128), CD94-APC (HP-3D9), CD158a-FITC (HP-3E4), CD158b-FITC (CH-L), HLA-DR-APC-Cy7 (L243), NKG2D-APC (1D11), perforin-FITC (δG9), granzyme A–FITC (CB9), Ki-67–FITC (B56), and IFN-γ–FITC (25723.11; BD); Vδ2-FITC (IMMU389), NKG2A-PE (Z199), CD3-ECD (UCHT1), and CD28-ECD (CD28.2; Beckman Coulter); Vδ1-FITC (TS1; Thermo Fisher Scientific); NKG2C-APC (134591; R&D Systems); CX3CR1-PE (2A9-1; MBL International); and T-bet–PE (4B10; eBioscience). Vγ5-PC5 (IMMU360) and Vδ3-FITC (P11.5B) were derived from Beckman Coulter via custom design service. Vγ2/3/4-biotin and Vγ2/3/4-FITC (23D12), Vγ4-FITC, Vγ5/3-biotin (56.3), and Vγ8-biotin (R4.5.1) were provided by D. Wesch (Institute of Immunology, University of Kiel, Kiel, Germany; Kabelitz et al., 1994; Hinz et al., 1997; Wesch et al., 1998). KLRG1–Alexa Fluor 488 (13F12F2) was provided by H. Pircher (University of Freiburg, Freiburg, Germany; Marcolino et al., 2004) and unlabeled Vδ3 antibody by E. Scotet (Institut National de la Santé et de la Recherche Médicale U601, Nantes, France; Peyrat et al., 1995). Staining was done on whole blood. Red blood cells were lysed using FACS Lysing solution (BD). The absolute number of γδ T cells in whole blood was determined using Trucount beads (BD). Intracellular staining for perforin-FITC, granzyme A–FITC, and Ki-67–FITC was performed with the Perm 2 kit (BD) and for T-bet–PE with the Foxp3 staining buffer set (eBioscience). For the detection of IFN-γ, PBMCs were stimulated for 4 h with 10 ng/ml PMA and 2 µM ionomycin in the presence of 2 µM monensin. Staining was done using the Cytofix/Cytoperm kit (BD). Cells were run on the CyAn flow cytometer equipped with three lasers (405, 488, and 633 nm) and data were analyzed using Summit 4.3 (Dako).

Microarray analysis.

PBMCs were isolated from cord blood by Lymphoprep gradient centrifugation (Axis-Shield). After depletion of remaining red blood cells and CD4+ cells by magnetic cell sorting (Miltenyi Biotec), CD3+γδ+ lymphocytes were sorted till high purity (>99%) with a MoFlo sorter (Dako). The γδ T cell yield varied from 80,000–300,000 cells per cord blood sample. Total RNA was isolated using the RNeasy Micro kit (QIAGEN) from sorted γδ T cells derived from three CMV-infected newborns and three CMV-uninfected newborns. RNA concentration was measured using the NanoDrop (Thermo Fisher Scientific) and RNA quality was assessed using the Bioanalyzer 2100 (Agilent Technologies). RNA was amplified into biotin-labeled complementary RNA (cRNA) by one-round in vitro transcription using the Premier kit (Applied Biosystems). The cRNA was fragmented and hybridized on the Human Genome U133 Plus 2.0 GeneChip (Affymetrix). Staining and scanning was done on the Affymetrix platform. The procedures, from RNA quality control to generation of raw data (CEL files), were performed at DNAVision (Gosselies, Belgium). The raw data were analyzed using the Affy package of Limma (linear models for microarray data; www.bioconductor.org), including fitting a linear model (lmfit) as described previously (Vermijlen et al., 2007). M- and A-values for each gene were generated. M (log2 of the fold change) is related to the degree of differential expression between the γδ T cells from CMV-infected newborns versus γδ T cells from CMV-uninfected newborns, whereas A is a measurement of the mean signal intensity. Genes were regarded as differentially expressed if the absolute M-value was >0.5 with a p-value <0.05. Genes with M-values >0.5 are enriched in the γδ T cells derived from CMV-infected newborns, whereas genes with M-values <−0.5 are enriched in the γδ T cells derived from CMV-uninfected newborns. The Database for Annotation, Visualization and Integrated Discovery (DAVID; http://david.abcc.ncifcrf.gov/) was used to assist in the discovery of functionally related groups of differentially expressed genes. Microarray data and procedures were deposited at Array Express (www.ebi.ac.uk/arrayexpress) under accession no. E-MEXP-2055.

Spectratyping.

Total RNA was isolated from PBMC of cord bood of CMV-infected newborns and CMV-uninfected newborns, after which cDNA was generated using the First Strand cDNA synthesis kit (Fermentas). PCR (40 cycles) was performed with Cδ (5′-GTAGAATTCCTTCACCAGACAAG-3′) and Vδ1 (5′-CTGTCAACTTCAAGAAAGCAGCGAAATC-3′) or Vδ2 (5′-ATACCGAGAAAAGGACATCTATG-3′) primers, resulting in amplification of the sequences containing the CDR3δ1 or CDR3δ2, respectively. For amplification of sequences containing the CDR3γ8, PCR was performed with Cγ (5′-CAAGAAGACAAAGGTATGTTCCAG-3′) and Vγ8 (5′-GCAAGCACAGGGAAGAGCCTTAA-3′). Then a run-off reaction (one cycle) was performed using the fluorescently labeled Cδ-FAM primer (5′-ACGGATGGTTTGGTATGAGGCTGA-3′) for CDR3δ1 and CDR3δ2 and with the Cγ-FAM primer (5′-CTTCTGGAGYTTTGTTTCAGC-3′) for CDR3γ8 (Déchanet et al., 1999; www.imgt.org). The labeled reaction products were run on a capillary sequencer (ABI3730xl or ABI3130xl analyzer) at DNAVision. The fluorescence intensity was analyzed using Peak Scanner 1.0 (Applied Biosystems). The index of oligoclonality was calculated as described previously (Déchanet et al., 1999; Pitard et al., 2008).

Sequencing.

As described in Spectratyping, PCR (40 cycles) was performed on cDNA to amplify the sequences that contain the CDR3δ1, CDR3δ2, or CDR3γ8. PCR products were TA cloned according to the instructions of the manufacturer (Invitrogen). Sequencing was performed on recombinant plasmids purified from bacterial clones by cycle sequencing (BigDye kit; Applied Biosystems). Electrophoresis of the sequencing reaction products was performed on the 96-capillary 3730xl DNA analyzer (Applied Biosystems) at DNAVision. The CDR3 length, V-gene, P/N nucleotides, D gene segments, and J gene segments were determined using the IMGT/V-QUEST tool (www.imgt.org; Brochet et al., 2008). The CDR3 is delimited by (but does not include) the anchor positions 2nd-Cys(C) 104 and J-PHE(F) 118. Only sequences in frame were included in Tables S2, S3, and S4.

Generation of γδ T cell clones.

γδ T cells (Vδ1+ or Vγ9+Vδ2+) from CMV-infected and CMV-uninfected newborns were sorted into wells at 1, 3, or 10 cells/well in X-VIVO 15 medium (Lonza) containing 10% fetal calf serum (PAA Laboratories), penicillin (100 U/ml), streptomycin (100 U/ml), (Lonza), and 2.5 µg/ml fungizone (Invitrogen) and stimulated with 4 µg/ml PHA-P (Sigma-Aldrich) and irradiated feeder cells (mix of two allogeneic PBMCs [100,000 cells/well] and irradiated B cell line JY [10,000 cells/well; Vanhecke et al., 1995; Halary et al., 2005; Gibbons et al., 2009]). At day 3, T cell growth factor (ZeptoMetrix) was added until it reached a final concentration of 5% of the medium, and at day 10, again, feeder cells and PHA were added. Restimulation with PHA/feeder cells was performed every 2–3 wk. 25 ng/ml IL-15 and 10 ng/ml IL-7(R&D Systems) were added to maintain expanded γδ T cell clones.

Coincubation of γδ T cell clones with CMV-infected target cells.

Confluent monolayers of the human embryonic lung fibroblasts (HEL299; American Type Culture Collection) in flat-bottom 96-well plates were incubated with CMV TB40/E strain (gift from Z. Tabi, Cardiff School of Medicine, Cardiff, UK; Tabi et al., 2001) at a multiplicity of infection (MOI) of 0.1 or 0.01 for 2 h, washed, and cultured for 5 d. Before coincubation with γδ T cell clones, the infected and uninfected fibroblasts were washed two times with PBS. Verification of infection was performed by evaluating cytopathic effect by microscopy and analyzing the expression of immediate early antigen by flow cytometry (antibody clone E13; Argen). γδ T cells were preincubated with either control IgG2a or anti-CD3 antibody (clone OKT3; eBioscience) for 10 min at 10 µg/ml. The antibodies remained present during the coincubation at 5 µg/ml. Treatment with soluble OKT3 did not influence the viability of the clones. γδ T cell clones were added at 30,000 cells/well and, after 6 h, supernatant was collected. Release of IFN-γ into the supernatant was quantified by ELISA (Invitrogen). The killing assay was performed as described previously (Vermijlen et al., 2002) with some modifications. Fibroblasts with [methyl-3H]thymidine-labeled DNA were infected with CMV for 5 d and coincubated with γδ T cells at the indicated effector to target ratios. After 4 h of coincubation, the level of DNA fragmentation induced by the γδ T cells in the fibroblasts was determined as previously described (Vermijlen et al., 2002).

CMV replication assay.

Confluent monolayers of human embryonic lung fibroblasts (HEL299) in flat-bottom 96-well plates were incubated with CMV (TB40/E) for 2 h (MOI 0.1), washed, and incubated with medium alone, with a public Vγ8Vδ1 clone or with a control Vγ9Vδ2 clone (150,000 cells per well). After 7 d, the quantity of infectious CMV from the supernatant was determined in quadruplicate by standard plaque assay titration (in plaque forming units).

Statistical analysis.

Differences between CMV-infected newborns and CMV-uninfected newborns were determined using the nonparametric Mann-Whitney test using InStat software (GraphPad Software, Inc.). Differences were regarded as significant at P < 0.05.

Online supplemental material.

Fig. S1 shows the Vγ chain expression of CMV-infected and CMV-uninfected newborns. Fig. S2 shows the association of the late differentiation phenotype of γδ T cells with the expression of cytotoxic mediators and chemokine receptor CX3CR1. Fig. S3 shows the CDR3δ2 repertoire. Fig. S4 shows TCR/CD3-dependent IFN-γ production by more public Vγ8Vδ1 clones upon coincubation with CMV-infected target cells. Table S1 provides an overview of differentially expressed genes in γδ T cells from CMV-infected newborns versus CMV-uninfected newborns. Tables S2–S4 contain the sequencing data for CDR3δ1, CDR3δ2, and CDR3γ8 of CMV-infected and CMV-uninfected newborns. Online supplemental material is available at http://www.jem.org/cgi/content/full/jem.20090348/DC1.

Acknowledgments

We are grateful to all the mothers for participating in this study. We would like to thank Sandra Lecomte for sample and data management, Frederic Lhommé for cell sorting, Muriel Stubbe and Binita Dutta for fruitful discussions, and Julie Déchanet-Merville, Bart Vandekerckhove, and Yasmin Haque for tips on cloning T cells. We are grateful to Daniela Wesch for providing antibodies directed against different Vγ chains of the VγI family, and we would like to thank Hanspeter Pircher for the KLRG1–Alexa Fluor 488 antibody, Emmanuel Scotet for the unlabeled Vδ3 antibody, and Zsuzsanna Tabi for providing the CMV strain TB40/E.

This work was supported by the Belgian Science Policy (return grant to D. Vermijlen and Interuniversity Attraction Pole), European Commission (FP6), National Fund for Scientific Research (FNRS), Government of the Walloon Region, and GSK Biologicals. A. Marchant is a senior research associate of the FNRS.

The authors have no conflicting financial interests.

Footnotes

Abbreviations used:

CDR3
complementary-determining-region-3
KIR
killer immunoglobulin receptor
MFI
mean fluorescence intensity
NKR
NK receptor

References

  • Adams E.J., Chien Y.H., Garcia K.C. 2005. Structure of a gammadelta T cell receptor in complex with the nonclassical MHC T22. Science. 308:227–231 10.1126/science.1106885 [PubMed] [Cross Ref]
  • Andrade F., Fellows E., Jenne D.E., Rosen A., Young C.S. 2007. Granzyme H destroys the function of critical adenoviral proteins required for viral DNA replication and granzyme B inhibition. EMBO J. 26:2148–2157 10.1038/sj.emboj.7601650 [PubMed] [Cross Ref]
  • Appay V., Dunbar P.R., Callan M., Klenerman P., Gillespie G.M., Papagno L., Ogg G.S., King A., Lechner F., Spina C.A., et al. 2002. Memory CD8+ T cells vary in differentiation phenotype in different persistent virus infections. Nat. Med. 8:379–385 10.1038/nm0402-379 [PubMed] [Cross Ref]
  • Battistini L., Borsellino G., Sawicki G., Poccia F., Salvetti M., Ristori G., Brosnan C.F. 1997. Phenotypic and cytokine analysis of human peripheral blood gamma delta T cells expressing NK cell receptors. J. Immunol. 159:3723–3730 [PubMed]
  • Beldjord K., Beldjord C., Macintyre E., Even P., Sigaux F. 1993. Peripheral selection of Vδ1+ cells with restricted T cell receptor δ gene junctional repertoire in the peripheral blood of healthy donors. J. Exp. Med. 178:121–127 10.1084/jem.178.1.121 [PMC free article] [PubMed] [Cross Ref]
  • Bolovan-Fritts C.A., Trout R.N., Spector S.A. 2004. Human cytomegalovirus-specific CD4+-T-cell cytokine response induces fractalkine in endothelial cells. J. Virol. 78:13173–13181 10.1128/JVI.78.23.13173-13181.2004 [PMC free article] [PubMed] [Cross Ref]
  • Bovenschen N., de Koning P.J., Quadir R., Broekhuizen R., Damen J.M., Froelich C.J., Slijper M., Kummer J.A. 2008. NK cell protease granzyme M targets alpha-tubulin and disorganizes the microtubule network. J. Immunol. 180:8184–8191 [PubMed]
  • Brandes M., Willimann K., Bioley G., Lévy N., Eberl M., Luo M., Tampé R., Lévy F., Romero P., Moser B. 2009. Cross-presenting human gammadelta T cells induce robust CD8+ alphabeta T cell responses. Proc. Natl. Acad. Sci. USA. 106:2307–2312 10.1073/pnas.0810059106 [PubMed] [Cross Ref]
  • Brochet X., Lefranc M.P., Giudicelli V. 2008. IMGT/V-QUEST: the highly customized and integrated system for IG and TR standardized V-J and V-D-J sequence analysis. Nucleic Acids Res. 36:W503–W508 10.1093/nar/gkn316 [PMC free article] [PubMed] [Cross Ref]
  • Caccamo N., Sireci G., Meraviglia S., Dieli F., Ivanyi J., Salerno A. 2006. gammadelta T cells condition dendritic cells in vivo for priming pulmonary CD8 T cell responses against Mycobacterium tuberculosis. Eur. J. Immunol. 36:2681–2690 10.1002/eji.200636220 [PubMed] [Cross Ref]
  • Cairo C., Mancino G., Cappelli G., Pauza C.D., Galli E., Brunetti E., Colizzi V. 2008. Vdelta2 T-lymphocyte responses in cord blood samples from Italy and Côte d’Ivoire. Immunology. 124:380–387 10.1111/j.1365-2567.2007.02784.x [PubMed] [Cross Ref]
  • Chen L., He W., Kim S.T., Tao J., Gao Y., Chi H., Intlekofer A.M., Harvey B., Reiner S.L., Yin Z., et al. 2007. Epigenetic and transcriptional programs lead to default IFN-gamma production by gammadelta T cells. J. Immunol. 178:2730–2736 [PubMed]
  • Chien Y.H., Konigshofer Y. 2007. Antigen recognition by gammadelta T cells. Immunol. Rev. 215:46–58 10.1111/j.1600-065X.2006.00470.x [PubMed] [Cross Ref]
  • Chowdhury D., Lieberman J. 2008. Death by a thousand cuts: granzyme pathways of programmed cell death. Annu. Rev. Immunol. 26:389–420 10.1146/annurev.immunol.26.021607.090404 [PMC free article] [PubMed] [Cross Ref]
  • Conti L., Casetti R., Cardone M., Varano B., Martino A., Belardelli F., Poccia F., Gessani S. 2005. Reciprocal activating interaction between dendritic cells and pamidronate-stimulated gammadelta T cells: role of CD86 and inflammatory cytokines. J. Immunol. 174:252–260 [PubMed]
  • Dalle J.H., Menezes J., Wagner E., Blagdon M., Champagne J., Champagne M.A., Duval M. 2005. Characterization of cord blood natural killer cells: implications for transplantation and neonatal infections. Pediatr. Res. 57:649–655 10.1203/01.PDR.0000156501.55431.20 [PubMed] [Cross Ref]
  • Davis M.M., Boniface J.J., Reich Z., Lyons D., Hampl J., Arden B., Chien Y. 1998. Ligand recognition by alpha beta T cell receptors. Annu. Rev. Immunol. 16:523–544 10.1146/annurev.immunol.16.1.523 [PubMed] [Cross Ref]
  • Day E.K., Carmichael A.J., ten Berge I.J., Waller E.C., Sissons J.G., Wills M.R. 2007. Rapid CD8+ T cell repertoire focusing and selection of high-affinity clones into memory following primary infection with a persistent human virus: human cytomegalovirus. J. Immunol. 179:3203–3213 [PubMed]
  • De Libero G. 1999. Control of gammadelta T cells by NK receptors. Microbes Infect. 1:263–267 10.1016/S1286-4579(99)80043-4 [PubMed] [Cross Ref]
  • De Rosa S.C., Andrus J.P., Perfetto S.P., Mantovani J.J., Herzenberg L.A., Herzenberg L.A., Roederer M. 2004. Ontogeny of gamma delta T cells in humans. J. Immunol. 172:1637–1645 [PubMed]
  • Déchanet J., Merville P., Lim A., Retière C., Pitard V., Lafarge X., Michelson S., Méric C., Hallet M.M., Kourilsky P., et al. 1999. Implication of gammadelta T cells in the human immune response to cytomegalovirus. J. Clin. Invest. 103:1437–1449 10.1172/JCI5409 [PMC free article] [PubMed] [Cross Ref]
  • Devilder M.C., Maillet S., Bouyge-Moreau I., Donnadieu E., Bonneville M., Scotet E. 2006. Potentiation of antigen-stimulated V gamma 9V delta 2 T cell cytokine production by immature dendritic cells (DC) and reciprocal effect on DC maturation. J. Immunol. 176:1386–1393 [PubMed]
  • Dieli F., Vermijlen D., Fulfaro F., Caccamo N., Meraviglia S., Cicero G., Roberts A., Buccheri S., D’Asaro M., Gebbia N., et al. 2007. Targeting human gammadelta T cells with zoledronate and interleukin-2 for immunotherapy of hormone-refractory prostate cancer. Cancer Res. 67:7450–7457 10.1158/0008-5472.CAN-07-0199 [PubMed] [Cross Ref]
  • Dollard S.C., Grosse S.D., Ross D.S. 2007. New estimates of the prevalence of neurological and sensory sequelae and mortality associated with congenital cytomegalovirus infection. Rev. Med. Virol. 17:355–363 10.1002/rmv.544 [PubMed] [Cross Ref]
  • Eberl M., Engel R., Aberle S., Fisch P., Jomaa H., Pircher H. 2005. Human Vgamma9/Vdelta2 effector memory T cells express the killer cell lectin-like receptor G1 (KLRG1). J. Leukoc. Biol. 77:67–70 [PubMed]
  • Eberl M., Roberts G.W., Meuter S., Williams J.D., Topley N., Moser B. 2009. A rapid crosstalk of human gammadelta T cells and monocytes drives the acute inflammation in bacterial infections. PLoS Pathog. 5:e1000308 10.1371/journal.ppat.1000308 [PMC free article] [PubMed] [Cross Ref]
  • Gibbons D.L., Haque S.F., Silberzahn T., Hamilton K., Langford C., Ellis P., Carr R., Hayday A.C. 2009. Neonates harbour highly active gammadelta T cells with selective impairments in preterm infants. Eur. J. Immunol. 39:1794–1806 10.1002/eji.200939222 [PubMed] [Cross Ref]
  • Goriely S., Van Lint C., Dadkhah R., Libin M., De Wit D., Demonté D., Willems F., Goldman M. 2004. A defect in nucleosome remodeling prevents IL-12(p35) gene transcription in neonatal dendritic cells. J. Exp. Med. 199:1011–1016 10.1084/jem.20031272 [PMC free article] [PubMed] [Cross Ref]
  • Halary F., Pitard V., Dlubek D., Krzysiek R., de la Salle H., Merville P., Dromer C., Emilie D., Moreau J.F., Déchanet-Merville J. 2005. Shared reactivity of Vδ2neg γδ T cells against cytomegalovirus-infected cells and tumor intestinal epithelial cells. J. Exp. Med. 201:1567–1578 10.1084/jem.20041851 [PMC free article] [PubMed] [Cross Ref]
  • Hayday A.C. 2000. [gamma][delta] cells: a right time and a right place for a conserved third way of protection. Annu. Rev. Immunol. 18:975–1026 10.1146/annurev.immunol.18.1.975 [PubMed] [Cross Ref]
  • Hayday A.C. 2009. Gammadelta T cells and the lymphoid stress-surveillance response. Immunity. 31:184–196 10.1016/j.immuni.2009.08.006 [PubMed] [Cross Ref]
  • Hinz T., Wesch D., Halary F., Marx S., Choudhary A., Arden B., Janssen O., Bonneville M., Kabelitz D. 1997. Identification of the complete expressed human TCR V gamma repertoire by flow cytometry. Int. Immunol. 9:1065–1072 10.1093/intimm/9.8.1065 [PubMed] [Cross Ref]
  • Holtmeier W., Kabelitz D. 2005. gammadelta T cells link innate and adaptive immune responses. Chem. Immunol. Allergy. 86:151–183 10.1159/000086659 [PubMed] [Cross Ref]
  • Ismaili J., Olislagers V., Poupot R., Fournié J.J., Goldman M. 2002. Human gamma delta T cells induce dendritic cell maturation. Clin. Immunol. 103:296–302 10.1006/clim.2002.5218 [PubMed] [Cross Ref]
  • Kabelitz D., Ackermann T., Hinz T., Davodeau F., Band H., Bonneville M., Janssen O., Arden B., Schondelmaier S. 1994. New monoclonal antibody (23D12) recognizing three different V gamma elements of the human gamma delta T cell receptor. 23D12+ cells comprise a major subpopulation of gamma delta T cells in postnatal thymus. J. Immunol. 152:3128–3136 [PubMed]
  • Kabelitz D., Wesch D., He W. 2007. Perspectives of gammadelta T cells in tumor immunology. Cancer Res. 67:5–8 10.1158/0008-5472.CAN-06-3069 [PubMed] [Cross Ref]
  • Kersten C.M., McCluskey R.T., Boyle L.A., Kurnick J.T. 1996. Escherichia coli and Pseudomonas aeruginosa induce expansion of V delta 2 cells in adult peripheral blood, but of V delta 1 cells in cord blood. J. Immunol. 157:1613–1619 [PubMed]
  • Lafarge X., Merville P., Cazin M.C., Bergé F., Potaux L., Moreau J.F., Déchanet-Merville J. 2001. Cytomegalovirus infection in transplant recipients resolves when circulating gammadelta T lymphocytes expand, suggesting a protective antiviral role. J. Infect. Dis. 184:533–541 10.1086/322843 [PubMed] [Cross Ref]
  • Lanier L.L. 2008. Up on the tightrope: natural killer cell activation and inhibition. Nat. Immunol. 9:495–502 10.1038/ni1581 [PMC free article] [PubMed] [Cross Ref]
  • Lee H.H., Hoeman C.M., Hardaway J.C., Guloglu F.B., Ellis J.S., Jain R., Divekar R., Tartar D.M., Haymaker C.L., Zaghouani H. 2008. Delayed maturation of an IL-12–producing dendritic cell subset explains the early Th2 bias in neonatal immunity. J. Exp. Med. 205:2269–2280 10.1084/jem.20071371 [PMC free article] [PubMed] [Cross Ref]
  • Levy O. 2007. Innate immunity of the newborn: basic mechanisms and clinical correlates. Nat. Rev. Immunol. 7:379–390 10.1038/nri2075 [PubMed] [Cross Ref]
  • Lewis D.B., Wilson C.B. 2001. Developmental immunology and role of host defenses in fetal and neonatal susceptibility to infection. In Infectious Disease of the Fetus and Newborn Infant Remington J.S., Klein J.O., editors. , W.B. Saunders Company, Philadelphia, PA: 25–138
  • Lieberman J. 2003. The ABCs of granule-mediated cytotoxicity: new weapons in the arsenal. Nat. Rev. Immunol. 3:361–370 10.1038/nri1083 [PubMed] [Cross Ref]
  • Liesnard C., Donner C., Brancart F., Gosselin F., Delforge M.L., Rodesch F. 2000. Prenatal diagnosis of congenital cytomegalovirus infection: prospective study of 237 pregnancies at risk. Obstet. Gynecol. 95:881–888 10.1016/S0029-7844(99)00657-2 [PubMed] [Cross Ref]
  • Marchant A., Goldman M. 2005. T cell-mediated immune responses in human newborns: ready to learn? Clin. Exp. Immunol. 141:10–18 10.1111/j.1365-2249.2005.02799.x [PubMed] [Cross Ref]
  • Marchant A., Appay V., Van Der Sande M., Dulphy N., Liesnard C., Kidd M., Kaye S., Ojuola O., Gillespie G.M., Vargas Cuero A.L., et al. 2003. Mature CD8(+) T lymphocyte response to viral infection during fetal life. J. Clin. Invest. 111:1747–1755 [PMC free article] [PubMed]
  • Marcolino I., Przybylski G.K., Koschella M., Schmidt C.A., Voehringer D., Schlesier M., Pircher H. 2004. Frequent expression of the natural killer cell receptor KLRG1 in human cord blood T cells: correlation with replicative history. Eur. J. Immunol. 34:2672–2680 10.1002/eji.200425282 [PubMed] [Cross Ref]
  • Maródi L. 2006. Neonatal innate immunity to infectious agents. Infect. Immun. 74:1999–2006 10.1128/IAI.74.4.1999-2006.2006 [PMC free article] [PubMed] [Cross Ref]
  • Metkar S.S., Menaa C., Pardo J., Wang B., Wallich R., Freudenberg M., Kim S., Raja S.M., Shi L., Simon M.M., Froelich C.J. 2008. Human and mouse granzyme A induce a proinflammatory cytokine response. Immunity. 29:720–733 10.1016/j.immuni.2008.08.014 [PubMed] [Cross Ref]
  • Mold J.E., Michaëlsson J., Burt T.D., Muench M.O., Beckerman K.P., Busch M.P., Lee T.H., Nixon D.F., McCune J.M. 2008. Maternal alloantigens promote the development of tolerogenic fetal regulatory T cells in utero. Science. 322:1562–1565 10.1126/science.1164511 [PMC free article] [PubMed] [Cross Ref]
  • Morita C.T., Parker C.M., Brenner M.B., Band H. 1994. TCR usage and functional capabilities of human gamma delta T cells at birth. J. Immunol. 153:3979–3988 [PubMed]
  • Morita C.T., Jin C., Sarikonda G., Wang H. 2007. Nonpeptide antigens, presentation mechanisms, and immunological memory of human Vgamma2Vdelta2 T cells: discriminating friend from foe through the recognition of prenyl pyrophosphate antigens. Immunol. Rev. 215:59–76 10.1111/j.1600-065X.2006.00479.x [PubMed] [Cross Ref]
  • Parker C.M., Groh V., Band H., Porcelli S.A., Morita C., Fabbi M., Glass D., Strominger J.L., Brenner M.B. 1990. Evidence for extrathymic changes in the T cell receptor γ/δ repertoire. J. Exp. Med. 171:1597–1612 10.1084/jem.171.5.1597 [PMC free article] [PubMed] [Cross Ref]
  • Pennington D.J., Vermijlen D., Wise E.L., Clarke S.L., Tigelaar R.E., Hayday A.C. 2005. The integration of conventional and unconventional T cells that characterizes cell-mediated responses. Adv. Immunol. 87:27–59 10.1016/S0065-2776(05)87002-6 [PubMed] [Cross Ref]
  • Peyrat M.A., Davodeau F., Houde I., Romagné F., Necker A., Leget C., Cervoni J.P., Cerf-Bensussan N., Vié H., Bonneville M., Hallet M.M. 1995. Repertoire analysis of human peripheral blood lymphocytes using a human V delta 3 region-specific monoclonal antibody. Characterization of dual T cell receptor (TCR) delta-chain expressors and alpha beta T cells expressing V delta 3J alpha C alpha-encoded TCR chains. J. Immunol. 155:3060–3067 [PubMed]
  • Pitard V., Roumanes D., Lafarge X., Couzi L., Garrigue I., Lafon M.E., Merville P., Moreau J.F., Déchanet-Merville J. 2008. Long-term expansion of effector/memory Vdelta2-gammadelta T cells is a specific blood signature of CMV infection. Blood. 112:1317–1324 10.1182/blood-2008-01-136713 [PubMed] [Cross Ref]
  • Ramsburg E., Tigelaar R., Craft J., Hayday A. 2003. Age-dependent requirement for γδ T cells in the primary but not secondary protective immune response against an intestinal parasite. J. Exp. Med. 198:1403–1414 10.1084/jem.20030050 [PMC free article] [PubMed] [Cross Ref]
  • Romero V., Fellows E., Jenne D.E., Andrade F. 2009. Cleavage of La protein by granzyme H induces cytoplasmic translocation and interferes with La-mediated HCV-IRES translational activity. Cell Death Differ. 16:340–348 10.1038/cdd.2008.165 [PubMed] [Cross Ref]
  • Stagno S. 2001. Cytomegalovirus. In Infectious Diseases of the Fetus and Newborn Infants Remington J.S., Klein J.O., editors. , W.B. Saunders Company, Philadelphia, PA: 389–424
  • Tabi Z., Moutaftsi M., Borysiewicz L.K. 2001. Human cytomegalovirus pp65- and immediate early 1 antigen-specific HLA class I-restricted cytotoxic T cell responses induced by cross-presentation of viral antigens. J. Immunol. 166:5695–5703 [PubMed]
  • Toulon A., Breton L., Taylor K.R., Tenenhaus M., Bhavsar D., Lanigan C., Rudolph R., Jameson J., Havran W.L. 2009. A role for human skin–resident T cells in wound healing. J. Exp. Med. 206:743–750 10.1084/jem.20081787 [PMC free article] [PubMed] [Cross Ref]
  • Trautmann L., Rimbert M., Echasserieau K., Saulquin X., Neveu B., Déchanet J., Cerundolo V., Bonneville M. 2005. Selection of T cell clones expressing high-affinity public TCRs within Human cytomegalovirus-specific CD8 T cell responses. J. Immunol. 175:6123–6132 [PubMed]
  • van Leeuwen E.M., de Bree G.J., ten Berge I.J., van Lier R.A. 2006. Human virus-specific CD8+ T cells: diversity specialists. Immunol. Rev. 211:225–235 10.1111/j.0105-2896.2006.00379.x [PubMed] [Cross Ref]
  • Vanhecke D., Verhasselt B., Debacker V., Leclercq G., Plum J., Vandekerckhove B. 1995. Differentiation to T helper cells in the thymus. Gradual acquisition of T helper cell function by CD3+CD4+ cells. J. Immunol. 155:4711–4718 [PubMed]
  • Vermijlen D., Luo D., Froelich C.J., Medema J.P., Kummer J.A., Willems E., Braet F., Wisse E. 2002. Hepatic natural killer cells exclusively kill splenic/blood natural killer-resistant tumor cells by the perforin/granzyme pathway. J. Leukoc. Biol. 72:668–676 [PubMed]
  • Vermijlen D., Ellis P., Langford C., Klein A., Engel R., Willimann K., Jomaa H., Hayday A.C., Eberl M. 2007. Distinct cytokine-driven responses of activated blood gammadelta T cells: insights into unconventional T cell pleiotropy. J. Immunol. 178:4304–4314 [PubMed]
  • Wang L., Kamath A., Das H., Li L., Bukowski J.F. 2001. Antibacterial effect of human V gamma 2V delta 2 T cells in vivo. J. Clin. Invest. 108:1349–1357 [PMC free article] [PubMed]
  • Wang T., Gao Y., Scully E., Davis C.T., Anderson J.F., Welte T., Ledizet M., Koski R., Madri J.A., Barrett A., et al. 2006. Gamma delta T cells facilitate adaptive immunity against West Nile virus infection in mice. J. Immunol. 177:1825–1832 [PubMed]
  • Wesch D., Hinz T., Kabelitz D. 1998. Analysis of the TCR Vgamma repertoire in healthy donors and HIV-1-infected individuals. Int. Immunol. 10:1067–1075 10.1093/intimm/10.8.1067 [PubMed] [Cross Ref]
  • White G.P., Watt P.M., Holt B.J., Holt P.G. 2002. Differential patterns of methylation of the IFN-gamma promoter at CpG and non-CpG sites underlie differences in IFN-gamma gene expression between human neonatal and adult CD45RO- T cells. J. Immunol. 168:2820–2827 [PubMed]
  • Wilhelm M., Kunzmann V., Eckstein S., Reimer P., Weissinger F., Ruediger T., Tony H.P. 2003. Gammadelta T cells for immune therapy of patients with lymphoid malignancies. Blood. 102:200–206 10.1182/blood-2002-12-3665 [PubMed] [Cross Ref]
  • Wilkinson G.W., Tomasec P., Stanton R.J., Armstrong M., Prod’homme V., Aicheler R., McSharry B.P., Rickards C.R., Cochrane D., Llewellyn-Lacey S., et al. 2008. Modulation of natural killer cells by human cytomegalovirus. J. Clin. Virol. 41:206–212 10.1016/j.jcv.2007.10.027 [PMC free article] [PubMed] [Cross Ref]
  • Yin Z., Chen C., Szabo S.J., Glimcher L.H., Ray A., Craft J. 2002. T-Bet expression and failure of GATA-3 cross-regulation lead to default production of IFN-gamma by gammadelta T cells. J. Immunol. 168:1566–1571 [PubMed]

Articles from The Journal of Experimental Medicine are provided here courtesy of The Rockefeller University Press