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      Skin infection generates non-migratory memory CD8+ T RM cells providing global skin immunity

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          Abstract

          Protective T cell memory has long been thought to reside in blood and lymph nodes, but very recently, the concept of immune memory in peripheral tissues mediated by resident memory T cells (TRM) has been proposed 1–5 . Here we show that localized vaccinia virus (VACV) skin infection generates long-lived non-recirculating CD8+ skin TRM that reside within the entire skin. These skin TRM are potent effector cells, and are superior to circulating central memory T cells (TCM) at providing rapid long-term protection against cutaneous re-infection. We find that CD8+ T cells are rapidly recruited to skin after acute VACV infection. CD8+ T cell recruitment to skin is independent of CD4+ T cells and IFN-γ, but requires the expression of E- and P-selectin ligands by CD8+ T cells. Using parabiotic mice, we further show that circulating CD8+ TCM and skin resident CD8+ TRM are both generated after skin infection; however, CD8+ TCM recirculate between blood and LN while TRM remain in skin. Cutaneous CD8+ TRM produce effector cytokines and persist for at least 6 months after infection. Mice with CD8+ skin TRM rapidly cleared a subsequent re-infection with VACV whereas mice with circulating TCM but no skin TRM showed greatly impaired viral clearance, indicating that TRM provide vastly superior protection. Finally, we show that TRM generated as a result of localized VACV skin infection reside not only in the site of infection, but also populate the entire skin surface and remain present for many months. Repeated re-infections lead to progressive accumulation of highly protective TRMin non-involved skin. These findings have important implications for our understanding of protective immune memory at epithelial interfaces with the environment, and suggest novel strategies for vaccines that protect against tissue tropic organisms. CD8+ T cells play a pivotal role in anti-viral immunity in target tissues 6–9 . We infected the skin of control, CD4−/−, or CD4+ T cell-depleted mice with VACV and assessed VACV-specific pentamer+ CD8+ T cells 10 . Absence of CD4+ T cells did not impair either antigen-specific CD8+ T cell proliferation in dLN or subsequent accumulation in skin; in fact the latter was enhanced (Fig.1a, b). We then infected mice infused with OT-I (CD8+) and OT-II (CD4+) T cells with an ovalbumin-expressing VACV (VACV-Ova) 11 . After skin infection, both OT-I and OT-II cells proliferated similarly in dLN, and OT-I cells but not OT-II cells accumulated significantly in infected skin (though other CD4+ T cells showed some accumulation) (Supplementary Fig. 1 and Fig. 1c, d). Interestingly, OT-I cells accumulated in infected skin efficiently in the absence of either CD4+ T cells or IFN-γ (Fig. 1e, f), in contrast to a recently reported HSV vaginal infection model 12 . However, skin accumulation (but not LN proliferation) of OT-I cells from FucT IV/VII−/− mice, which cannot make E- and P-selectin ligands, was significantly impaired (Fig. 1g, Supplementary Fig. 2a). Both E- and P-selectin were significantly upregulated in VACV infected skin (Supplementary Fig. 2b). Thus, CD8+ T cell accumulation in skin after VACV infection does not require CD4+ T cells or IFN-γ, but does require expression of E- and P-selectin ligands. Murine models of viral infections of skin and other tissues have been useful in the study of T cell memory 13–16 . We explored the ability of CD8+ memory T cells generated by VACV infection to recirculate following resolution of the cutaneous infection. We infected with VACV the skin of mice infused with OT-I cells, and waited until complete resolution of the infection (30 days). At 30 days we could identify TCM in LN and TEM in skin (Supplementary Fig. 3a, b). We then surgically created parabiotic pairs between the infected mice and never-infected naïve mice that had not been given OT-I cells. Parabiotic pairs were maintained for 2, 4, 8, 12, and 24 weeks, at which point they were surgically separated for the analysis of VACV-specific OT-I T cells (Fig. 2a). Mice joined for 2 weeks had similar numbers of OT-I TCM in the spleen and LN of both parabionts, indicating rapid recirculation and equilibration of TCM (Fig. 2b, d). However, at 2, 4, or 8 weeks there were no OT-I TRM in the skin of the unimmunized parabiont (Fig 2c, e). These early kinetics of TCM recirculation and TRM non-recirculation were confirmed by parabiotic mice that received no OT-I cells, using pentamer expression to identify VACV specific memory cells (Supplementary Fig. 4). OT-I TRM were readily identified in the skin of previously infected parabionts and mice that had been infected in parallel but never joined. These OT-I TRM represented a significant fraction of total skin cells (Fig. 2c), and persisted for long periods of time: 30% of skin CD8+ T cells at 12 weeks, and 15–20% of skin CD8+ T cells at 24 weeks. In contrast, naïve mice joined to previously infected mice had no OT-I TRM in the skin, even after 24 weeks of parabiosis (Fig. 2c, e). Thus, skin TRM persisted in skin for at least 6 months after infection and did not recirculate appreciably. TRM and TCM were further analyzed by FACS for expression of CD69, CD103, E- and P-selectin ligands, and production of IFN-γ and TNF-α upon activation. A subset of TRM expressed Bcl-2, and TRM lacked CD122 and CD127 (Supplementary Fig. 5). Immunofluorescence staining showed that many TRM localize in epidermal and follicular epithelium, as reported in skin HSV infection 17 , but also localize in the dermis (Fig. 2f). To directly compare the ability of TCM and TRM to eliminate a subsequent VACV infectious challenge, we infused µMT mice with OT-I cells and infected them via skin with VACV-Ova. After 30 days, mice were joined parabiotically to naïve µMT mice for 8 weeks, and then surgically separated. The infected parabiont contained TCM in both the spleen and LN and TRM within the skin, whereas the uninfected parabiont contained TCM only in the spleen and LN (Fig. 2). At 2 weeks after separation, the skin of these mice was challenged with VACV-Ova, and assessed 6 days later for viral load (Fig. 3a). Despite the presence of abundant circulating OT-I TCM, uninfected parabionts cleared virus only 30-fold more effectively than naïve mice (Fig. 3b). In contrast, the infected parabiont cleared the virus completely, 104-fold more effectively than the uninfected parabiont (Fig. 3b). Viral clearance was efficient even in mice treated with FTY720, a S1P inhibitor that blocks egress of TCM from LN into blood 1 (Fig. 3b). To prove that this was not an artifact of OT-I cell transfer, we reproduced and extended the experiment in a parabiotic model not involving transfer of OT-I cells (Fig. 3c). Parabiotic pairs were separated at 4 weeks, challenged with VACV, and assessed for viral load at 6, 14, and 26 days after challenge. There were again striking differences in the ability of endogenous TRM and TCM to mediate viral clearance at days 6 (Fig. 3d) and 14 (Fig 3e), which began to normalize by day 26 (Fig. 3f). However, FTY720 treated TCM mice are unable to clear virus even 26 days after infection, a time point by which naïve mice have cleared the skin infection (Fig. 3f), presumably by generating protective TRM. Thus, while TCM are superior to naïve T cells, they are inferior to TRM at mediating rapid viral clearance from skin. E- and P-selectin, CCL17, and ICAM-1 are expressed constitutively on the blood vessels of normal skin 18–20 and can support entry into uninflamed skin of TEM generated by cutaneous VACV infection. To study this phenomenon, we infected the left ears of OT-I-loaded mice with VACV-Ova and then measured the accumulation of OT-I cells in both infected (left) and uninfected (right) ears. There was measurable accumulation of OT-I cells in both ears, with similar kinetics. The absolute number of OT-I cells was always higher in the infected ear, but even 30 days after infection, OT-I cells represented a measurable fraction of all cells present in the uninfected ear (Fig. 4a). Thus, VACV skin infection generates CD8+ TRM that distribute to distant skin sites as well as the site of infection. The accumulation of OT-I TRM in distant skin sites is increased further after multiple sequential infections to other sites of skin (Fig. 4b-d), suggesting that skin TRM continue to accumulate throughout skin in response to repeated cutaneous infections at distant sites. To determine if CD8+ TRM in distant skin sites were protective as those at previously infected sites, we challenged µMT mice previously infected on one ear with a second VACV skin infection on both ears either 7 or 30 days after the initial infection. FYT720 was administered to limit the contribution of TCM (Fig. 4e). Strikingly, at both day 7 and day 30, TRM in distant skin sites dramatically reduced viral loads to levels comparable to those observed at the actual site of previous infection, indicating that these distant TRM cells were highly effective at rapidly eliminating virus. In contrast, viral loads in the skin of i.p. immunized mice were between 103 and 104 higher at these time points (Fig. 4f, g). Thus, skin infection with VACV generates populations of TEM that distribute to the entire skin surface, become TRM, and mediate protection of the skin against re-infection with VACV in the absence of antibodies or TCM. TRM have now been identified in the skin, gut, lung and brain in murine models 21–23 and human subjects in both health and in the setting of skin disease 4, 5, 24, 25 . We demonstrate that after VACV viral infection through skin, CD8+ TRM are generated and distribute not only to the site of infection but also throughout the entire skin surface. These CD8+ TRM produce effector cytokines, persist for many months, and are highly effective at rapidly controlling subsequent VACV skin infection. TRM were orders of magnitude more effective than TCM at controlling viral re-infection of the skin, at all time points examined in this study. The use of parabiotic mice allowed us to rigorously examine the tissue distribution and relative roles of TCM and TRM in VACV immune responses. The relatively minor role of CD4+ T cells in VACV skin infection may reflect differences in immune responses to different viruses and/or infection of different tissues, as CD4+ T cells are clearly more important in HSV infection 12, 26 . Moreover, CD4+ TRM cells predominate in human skin 24 and lung 25 , and are enriched for memory cells specific for pathogens encountered through those tissues 27, 28 . Pathogens typically invade the host through epithelial interfaces with the environment. Our studies suggest that TEM generated as a result of epithelial tissue infections accumulate as TRM at both sites of infection as well as at distant sites within the same epithelial tissue, providing broad and long-lived protective T cell immunity against re-infection. A more complete understanding TRM mediated immune memory should enhance our understanding of adaptive immunologic memory, influence rational vaccine design, and illuminate pathophysiology of human T cell mediated diseases. METHODS Mice C57BL/6, CD4−/−, IFN-γ−/− and µMT mice were purchased from The Jackson Laboratory. Thy1.1+ Rag−/− OT-I, CD45.1+ OT-II, FucT IV/VII−/− mice were housed at the animal facility of Harvard Institute of Medicine, Harvard Medical School. Thy1.1+ Rag−/− OT-I mice were crossed with FucT IV/VII−/− mice to yield Thy1.1+ FucT IV/VII−/− OT-I mice. OT-I and OT-II are T cell receptor-transgenic mice recognizing chicken ovalbumin residues 257–264 in the context of H2Kb and 323–339 in the context of I-Ab, respectively. Animal experiments were performed in accordance with the guidelines set out by the Center for Animal Resources and Comparative Medicine at Harvard Medical School. Viruses and Infections Recombinant VACV (Western Reserve strain) and VACV-Ova were originally obtained from Dr. Bernard Moss (NIH, Bethesda, MD) and grown on Hela cells. Viral titres were determined using CV-1 cells and 2×106 PFU of VACV or VACV-Ova was used for epicutaneous infection by skin scarification (s.s.) or intraperitoneal (i.p.) injection, as described previously 29 . Parabiotic mice Parabiosis surgery was performed as described elsewhere 30 with some modifications. Briefly, sex- and age-matched mouse partners were anesthetized to full muscle relaxation with ketamine and xylazine (10 µg/g) or with 2.5% avertin (15µl/g) by i.p. injection. The corresponding lateral aspects of mice were shaved and the excess hair was wiped off with alcohol prep pad. After skin disinfection by wiping with betadine solution and 70% ethanol three times, two matching skin incisions were made from the olecranon to the knee joint of each mouse, and the subcutaneous fascia was bluntly dissected to create about 1/2 cm of free skin. The olecranon and knee joints were attached by a single 5-0 silk suture and tie, and the dorsal and ventral skins were approximated by staples or continuous suture. Betadine solution was used to cover the full length of the dorsal and ventral incision. The mice were then kept on heating pads and continuously monitored until recovery. 2.5 µg/g Flunixin was used for analgesic treatment by subcutaneous injection every 8–12 hours for 48 hours post operation. After an interval of the indicated weeks, parabiotic mice were surgically separated by a reversal of the above procedure for the next experiments. Adoptive transfer and T cell depletion Lymph nodes were collected from the naïve female Thy1.1+ Rag−/− OT-I, CD45.1+ OT-II, or Thy1.1+ FucT IV/VII−/− OT-I mice at age of 6–8 weeks. OT-I or OT-II cells were purified by magnetic cell sorting using mouse CD8α+ or CD4+ T cell isolation kit (Miltenyi Biotec), respectively. 2×106 isolated OT-I and / or OT-II cells were then intravenously transferred to female recipient mice. In some experiments, OT-I and OT-II cells were labeled with carboxyfluorescein succinimidyl ester (CFSE) before co-transfer. To deplete CD4+ T cells in vivo, the recipient mice were injected i.p. with 500 µg anti-CD4 (GK1.5) in 100 µl PBS 4 days and 1 day before and on day 2 and 5 post infection. Preparation of cell suspensions LN and spleen were harvested and mashed through a 70 µm nylon cell strainer to prepare cell suspensions. Red blood cells were lysed using lysing buffer. Skin tissue was removed after hair removal, chopped into small fragments and incubated in HBSS supplemented with 1 mg/ml collagenase A and 40 µg/ml DNase I at 37°C for 30 min. After filtrating through a 70 µm nylon cell strainer, cells were collected and washed thoroughly with cold PBS before staining. Intracellular cytokine detection The infected skin from memory OT-I-bearing mice was harvested at 35 days after infection, and single cell suspension was prepared as described above. In some cases, 2 months after s.s. with VACV-Ova, mice transferred with low (2×104) or high (2×106) number of OT-I cells were i.p. challenged with VACV-Ova. 5 days after challenge, splenocytes were prepared. Red blood cells were lysed using lysing buffer. Cells were then incubated with 2 µg/ml SINFEKL peptide of ovabulmin at the presence of Brefeldin A for 7 hours. Fc receptors were blocked with CD16/CD32 mAbs and intracellular IFN-γ, TNF-α and IL-2 staining was performed using Intracellular Cytokine Detection Kits (BD Bioscience) before flow cytometry. Determination of viral load Mice were challenged with 2×106 PFU VACV or VACV-Ova on the skin. In some cases, mice were simultaneously injected (i.p.) with 1 µg/g FTY720 each day. At indicated time points, viral load of skin was examined by quantitative real-time PCR, as described previously 29 . Isolation of mRNA and real-time PCR Total RNA was extracted from homogenized skin tissue and cDNA was generated with iScript cDNA synthesis kit (Bio-Rad). Bio-Rad iCycler iQ Real-Time PCR Detection System (Bio-Rad) was used with the following settings: 45 cycles of 15 seconds of denaturation at 95°C, and 1 minute of primer annealing and elongation at 60°C. Real-time PCR was done with 1 µl cDNA plus 12.5 µl of 2× iQ™ SYBR Green Supermix (Bio-Rad) and 0.5 µl (10 µM) specific primers: mE-selectin 1 (5′-GGA CAC CAC AAA TCC CAG TCT G-3′) and mE-selectin 2 (5′- TCG CAG GAG AAC TCA CAA CTG G-3′); mP-selectin 1 (5′-AAG ATG CCT GGC TAC TGG ACA C-3′) and mP-selecin 2 (5′-CAA GAG GCT GAA CGC AGG TCA T-3′); mβ-actin 1 (5’-CAT TGC TGA CAG GAT GCA GAA GG-3’) and mβ-actin 2 (5’-TGC TGG AAG GTG GAC AGT GAG G-3’). All samples were run in duplicate and fold change of gene expression was calculated using the reference sample (naïve skin). Antibodies and flow cytometry The following anti-mouse antibodies were obtained from BD PharMingen: CD8a (53-6.7), Thy1.1 (OX-7), CD4 (L3T4), CD45.1 (A20), CD19 (1D3), CD16/CD32 (2.4G2), CD44 (IM7), CD62L (MEL-14), CD69 (H1.2F3), CD103 (M290), CD122 (TM-Beta 1), Bcl-2 (A19-3), α4β7 (DATK32), IFN-γ (XMG1.2), TNF-α (MP6-XT22), IL-2 (JES6-5H4). Fluorescence-conjugated anti-mouse CD127 (A7R34) and PD-1 (RMP1-30) were purchased from eBioscience. PE-conjugated B8R20–27/H-2Kb pentamers were obtained from ProImmune Ltd and pentamer+ CD8+ T cell staining was performed according to the protocol provided by company. E- or P-selectin ligand expression was examined by incubating cells with rmE-Selectin/Fc Chimera or rmP-Selectin/Fc Chimera (R&D System) in conjunction with APC-conjugated F(ab')2 fragments of goat anti-human IgG F(c) antibody (Jackson Immunoresearch). Dead cells were excluded using 7-AAD staining. Data were analyzed on FACSCantoTM Flow Cytometer using FACSDiva software. Immunofluorescence Microscopy 1 cm tail containing the infected skin site from OT-I-bearing mice was harvested and deboned at 45 days after s.s. with VACV-Ova. The skin was collected and embedded in OCT (Tissue-Tek; Sakura) and frozen at −80°C. Skin sections were performed on a cryostat (Leica CM1850 UV) at 6-µm thickness and air-dried for 6–8 hours. Sections were then fixed in −20°C acetone for 5 min, rehydrated with PBS properly, and blocked with 2% FCS in PBS for 15 min at room temperature (RT, 20°C). After staining with Thy1.1-PE (1:200) in PBS for 1 hour at RT, sections were rinsed 3 times (5 min/time) with TBS-tween 20 by properly shaking and mounted with DAPI Fluoromount-G (Southern Biotech, Alabama, USA). Images were acquired with a Nikon Eclipse E600 microscope and processed using SPOTSOFTWARE (version 4.6, Diagnostic Instruments, Inc.). Statistical analysis Statistical significance in values between experimental groups was determined by one-way analysis of variance (ANOVA) followed by Tukey post-test. P<0.05 was considered statistically significant. Supplementary Material 1

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          Most cited references 19

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          Different patterns of peripheral migration by memory CD4+ and CD8+ T cells.

          Infections localized to peripheral tissues such as the skin result in the priming of T-cell responses that act to control pathogens. Activated T cells undergo migrational imprinting within the draining lymph nodes, resulting in memory T cells that provide local and systemic protection. Combinations of migrating and resident memory T cells have been implicated in long-term peripheral immunity, especially at the surfaces that form pathogen entry points into the body. However, T-cell immunity consists of separate CD4(+) helper T cells and CD8(+) killer T cells, with distinct effector and memory programming requirements. Whether these subsets also differ in their ability to form a migrating pool involved in peripheral immunosurveillance or a separate resident population responsible for local infection control has not been explored. Here, using mice, we show key differences in the migration and tissue localization of memory CD4(+) and CD8(+) T cells following infection of the skin by herpes simplex virus. On resolution of infection, the skin contained two distinct virus-specific memory subsets; a slow-moving population of sequestered CD8(+) T cells that were resident in the epidermis and confined largely to the original site of infection, and a dynamic population of CD4(+) T cells that trafficked rapidly through the dermis as part of a wider recirculation pattern. Unique homing-molecule expression by recirculating CD4(+) T effector-memory cells mirrored their preferential skin-migratory capacity. Overall, these results identify a complexity in memory T-cell migration, illuminating previously unappreciated differences between the CD4(+) and CD8(+) subsets.
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            Little evidence for developmental plasticity of adult hematopoietic stem cells.

            To rigorously test the in vivo cell fate specificity of bone marrow (BM) hematopoietic stem cells (HSCs), we generated chimeric animals by transplantation of a single green fluorescent protein (GFP)-marked HSC into lethally irradiated nontransgenic recipients. Single HSCs robustly reconstituted peripheral blood leukocytes in these animals, but did not contribute appreciably to nonhematopoietic tissues, including brain, kidney, gut, liver, and muscle. Similarly, in GFP+:GFP- parabiotic mice, we found substantial chimerism of hematopoietic but not nonhematopoietic cells. These data indicate that "transdifferentiation" of circulating HSCs and/or their progeny is an extremely rare event, if it occurs at all.
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              Heterogeneity and cell-fate decisions in effector and memory CD8+ T cell differentiation during viral infection.

              Heterogeneity is a hallmark of the adaptive immune system. This is most evident in the enormous diversity of B and T cell antigen receptors. There is also heterogeneity within antiviral T cell populations, and subsets of effector and memory T cells now permeate our thinking about specialization of T cell responses to pathogens. It has been less clear, however, how heterogeneity in developing virus-specific effector and memory T cells is related to cell-fate decisions in the immune response, such as the generation long-lived memory T cells. Here we discuss recent findings that might help redefine how heterogeneity in antiviral T cell populations gives rise to T cell subsets with short- and long-lived cell fates.
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                Author and article information

                Journal
                0410462
                6011
                Nature
                Nature
                Nature
                0028-0836
                1476-4687
                6 August 2012
                29 February 2012
                10 September 2012
                : 483
                : 7388
                : 227-231
                Affiliations
                [1 ]Department of Dermatology and Harvard Skin Disease Research Center, Brigham and Women’s Hospital, Harvard Medical School, Boston, MA 02115, USA
                [2 ]Department of Stem Cell and Regenerative Biology, Harvard University, Howard Hughes Medical Institute, Harvard Stem Cell Institute, Joslin Diabetes Center, Boston, MA 02115, USA
                Author notes
                Correspondence and requests for materials should be addressed to T.S.K. ( tkupper@ 123456partners.org )
                Article
                nihpa349932
                10.1038/nature10851
                3437663
                22388819

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