|A germinal center-independent pathway generates unswitched memory B cells early in the primary response.|
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|PMID: 22370719 Owner: NLM Status: MEDLINE|
|Memory B cells can be produced from the classical germinal center (GC) pathway or a less understood GC-independent route. We used antigen-based cell enrichment to assess the relative contributions of these pathways to the polyclonal memory B cell pool. We identified a CD38(+) GL7(+) B cell precursor population that differentiated directly into IgM(+) or isotype-switched (sw) Ig(+) memory B cells in a GC-independent fashion in response to strong CD40 stimulation. Alternatively, CD38(+) GL7(+) B cell precursors had the potential to become Bcl-6(+) GC cells that then generated primarily swIg(+) memory B cells. These results demonstrate that early IgM(+) and swIg(+) memory B cells are products of a GC-independent pathway, whereas later switched Ig(+) memory B cells are products of GC cells.|
|Justin J Taylor; Kathryn A Pape; Marc K Jenkins|
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|Type: Journal Article; Research Support, N.I.H., Extramural Date: 2012-02-27|
|Title: The Journal of experimental medicine Volume: 209 ISSN: 1540-9538 ISO Abbreviation: J. Exp. Med. Publication Date: 2012 Mar|
|Created Date: 2012-03-13 Completed Date: 2012-05-08 Revised Date: 2013-06-26|
Medline Journal Info:
|Nlm Unique ID: 2985109R Medline TA: J Exp Med Country: United States|
|Languages: eng Pagination: 597-606 Citation Subset: IM|
|Department of Microbiology, Center for Immunology, University of Minnesota Medical School, Minneapolis, MN 55455, USA. TAYL0611@umn.edu|
|APA/MLA Format Download EndNote Download BibTex|
Antigens, CD38 / metabolism
Antigens, CD40 / administration & dosage
Antigens, Differentiation / metabolism
B-Lymphocyte Subsets / immunology*
DNA-Binding Proteins / deficiency, genetics, immunology
Germinal Center / immunology
Membrane Glycoproteins / metabolism
Mice, 129 Strain
Mice, Inbred C57BL
Multipotent Stem Cells / immunology
Receptors, Antigen, B-Cell / metabolism
Signal Transduction / immunology
|F32 AI091033/AI/NIAID NIH HHS; R01 AI036914/AI/NIAID NIH HHS; R37 AI027998/AI/NIAID NIH HHS; T32 CA009138/CA/NCI NIH HHS|
|0/Antigens, CD40; 0/Antigens, Differentiation; 0/Bcl6 protein, mouse; 0/DNA-Binding Proteins; 0/Membrane Glycoproteins; 0/Receptors, Antigen, B-Cell; 0/antigen GL7; EC 126.96.36.199/5'-Nucleotidase; EC 188.8.131.52/Antigens, CD38; EC 184.108.40.206/Cd38 protein, mouse|
|Am J Transplant. 2013 May;13(5):1117
Journal ID (nlm-ta): J Exp Med
Journal ID (hwp): jem
Publisher: The Rockefeller University Press
© 2012 Taylor et al.
Received Day: 12 Month: 8 Year: 2011
Accepted Day: 30 Month: 1 Year: 2012
Print publication date: Day: 12 Month: 3 Year: 2012
Volume: 209 Issue: 3
First Page: 597 Last Page: 606
PubMed Id: 22370719
Publisher Id: 20111696
|A germinal center–independent pathway generates unswitched memory B cells early in the primary response Alternate Title:Germinal center–independent memory response|
|Justin J. Taylor|
|Kathryn A. Pape|
|Marc K. Jenkins|
|Department of Microbiology, Center for Immunology, University of Minnesota Medical School, Minneapolis, MN 55455
|Correspondence: CORRESPONDENCE Justin J. Taylor: TAYL0611@umn.edu
Antibody-mediated immunity after primary infection or vaccination relies on the development and persistence of antigen-specific memory B cells and antibody-secreting plasma cells (MacLennan, 1994; McHeyzer-Williams and McHeyzer-Williams, 2005; Tarlinton, 2008; Maul and Gearhart, 2010). Plasma cells constitutively secrete antibody, which provides a first level of protection against infection with the original microbe. Plasma cells do not appear to respond to a second infection because of low surface expression of the membrane-bound version of Ig (BCR; Manz et al., 1998). Memory B cells, in contrast, maintain BCR expression and differentiate quickly into antibody-secreting cells after encountering the antigen a second time (Benson et al., 2009; Dogan et al., 2009; Pape et al., 2011).
Memory B cells are the progeny of rare naive B cells that express BCRs specific for the eliciting antigen. After antigen binding to the BCR and receipt of signals from helper T cells, naive B cells proliferate and undergo Ig isotype switching from IgM and IgD to IgG, IgA, or IgE (MacLennan, 1994; McHeyzer-Williams and McHeyzer-Williams, 2005; Tarlinton, 2008; Maul and Gearhart, 2010). The cells then differentiate into short-lived plasma cells that secrete antibodies, or germinal center (GC) cells, which then generate memory B cells and long-lived plasma cells (MacLennan, 1994; McHeyzer-Williams and McHeyzer-Williams, 2005; Tarlinton, 2008; Maul and Gearhart, 2010). Memory cells are selected in GC through a process involving acquisition of Ig somatic hypermutations that enhance antigen binding and allow successful competition for survival-promoting signals from helper T cells (MacLennan, 1994; McHeyzer-Williams and McHeyzer-Williams, 2005; Tarlinton, 2008; Maul and Gearhart, 2010).
Recent evidence, however, has posed challenges to this traditional model. First, several studies have noted the existence of memory B cells with IgM+ BCRs (Klein et al., 1997, 1998; Anderson et al., 2007; Dogan et al., 2009; Pape et al., 2011). Moreover, these IgM+ memory cells can outnumber the isotype-switched (swIg+) memory cells of the same specificity (Dogan et al., 2009; Pape et al., 2011). Second, memory B cells and GC cells appear simultaneously (Blink et al., 2005; Chan et al., 2009), whereas the model predicts that GC cells should arise first. Lastly, not all memory B cells have Ig somatic mutations (Schittek and Rajewsky, 1992; Anderson et al., 2007; Pape et al., 2011) and memory B cells can be detected in mice that cannot form GC (Toyama et al., 2002). Collectively, the data indicate that Ig isotype switching, somatic mutation, and GC selection are not required for memory cell generation. The GC-independent pathway of memory B cell formation, however, is not understood.
In this study, we assessed the contributions of the GC-dependent and -independent pathways of memory B cell formation using an antigen-based cell enrichment protocol that we recently developed (Pape et al., 2011). We focused on very early times in the primary response to identify the point at which the two pathways diverged. We found that GC-independent memory B cells were mainly CD73− and IgM+ and were derived directly from a multipotent precursor that also produced GC cells. GC cells then generated mainly swIg+ memory B cells, which could be identified by expression of CD73.
Naive B cells specific for a given antigen are difficult to detect because they are rare among the 200 × 106 nucleated cells in the secondary lymphoid organs of a mouse. To analyze all antigen-specific B cells in these organs by flow cytometry, we developed a cell enrichment protocol that concentrates of the relevant cells into a sample containing ∼106 cells (Pape et al., 2011). Using this method, we reported that 20,000 R-PE–specific and 4,000 allophycocyanin-specific B cells exist in the secondary lymphoid organs of individual C57BL/6 mice that had not been exposed to these antigens (Pape et al., 2011). In the same study, we tracked PE-specific memory and GC B cell formation from these naive precursors in the spleen and LN after s.c. immunization with PE emulsified in CFA.
Because the goal of the current study was to track GC-dependent and -independent memory cell formation, we examined various secondary lymphoid organs individually to get a better handle on the anatomy of the GC reaction in this system. As shown in Fig. 1 A, PE-specific naive B cells comprised a very small fraction of the total B cell population in an unenriched spleen and LN sample from an unimmunized B6 mouse. In contrast, the frequency of PE-specific B cells increased 21-fold over the starting frequency in the draining inguinal and periaortic LN 29 d after an s.c. injection of PE in CFA. The frequency of PE-specific B cells also increased in the spleen and nondraining LN, although only about fivefold. Enrichment with PE and anti-PE magnetic beads revealed a similar pattern of B cell clonal expansion while increasing the representation of PE-specific B cells in each sample. Analysis of the PE-specific B cells in the enriched samples showed that GC B cells (GL7+) were more frequent in the PE-specific B cell population in the draining LN, although some GC B cells were present in other locations (Fig. 1 B). These results highlight the utility of the antigen-based cell enrichment method and support the approach of pooling the spleen and LN to capture the maximal number of GC-dependent B cells.
A challenge for the early detection of memory B cells is the lack of a unique phenotypic marker that distinguishes these cells from naive B cells in mice. For example, both naive and memory B cells express the CD38+ GL7− phenotype. Memory B cells, however, can be identified as CD38+ GL7− B cells that divided in response to stimulation by antigen in the past. We tracked memory B cell formation using this criterion by transferring CFSE-labeled naive B cells from CD45.1+ donor animals into congenic CD45.2+ recipients. The gating used to detect CD45.1+ PE+ donor B cells is shown in Fig. 2 A. The great majority of PE-specific B cells remained CFSEhigh in unimmunized mice (Fig. 2 B) and proliferation was not induced after the injection of CFA alone (unpublished data). In contrast, CD45.1+ donor PE-specific B cells began to proliferate and lose CFSE between days 1 and 2 after injection of PE in CFA (Fig. 2 B) as observed in other immune responses (Chan et al., 2009; Coffey et al., 2009). Between days 2 and 4, the PE-specific CFSElow responding B cell population contained two subsets: CD38+ GL7− memory phenotype cells and CD38+ GL7+ cells (Fig. 2 C). The CD38+ GL7+ cells peaked at day 7 and declined rapidly thereafter (Fig. 2 D). CFSElow CD38+ GL7− memory B cells could be detected as early as day 3, with the majority of cells appearing between days 5 and 7 (Fig. 2 D). CD38− GL7+ GC B cells were not detected until day 5 but expanded robustly after that (Fig. 2 D). The absence of GC B cells before day 5 was not a limit of detection issue resulting from the adoptive transfer approach because similar kinetics were found when the total number of PE-specific GC B cells within the entire recipient animal was calculated (Fig. 2 E). Therefore, PE-specific CD38+ GL7+ B cells appeared at the same time as early CD38+ GL7− memory B cells and before CD38− GL7+ GC B cells.
Immunohistology was performed to further test the possibility that CD38+ GL7+ B cells form before GC B cells. As shown in Fig. 3 A, a few GL7− naive PE-specific B cells were detected at random locations in the follicles of mice that were not injected with PE. By day 4 after injection of PE in CFA, PE-specific B cells had increased in number. The majority of these cells (80%) were located at the T/B border, whereas most of the remaining cells were in the follicles (Fig. 3 B). About 30% of the PE-specific B cells expressed GL7 on day 4 and all of these cells were located at the T/B border (Fig. 3, B–F). Nascent GCs were beginning to form at this time, but no PE-specific B cells were present in these structures (Fig. 3 B). In contrast, PE-specific B cells dominated the GCs at day 14 (Fig. 3 G). This in situ approach therefore confirmed the conclusion that CD38+ GL7+ B cells arise before GC B cells.
We sought to determine the relationship of the CD38+ GL7+ B cells to memory B cells and later GC B cells. A similar population of CD38+ B cells expressing the GC marker PNA has been hypothesized to be an early GC B cell (Shinall et al., 2000). In addition, Schwickert et al. (2011) found GL7+ CCR6+ FAS+ B cells at the border between the T cell areas and follicles of the draining LN and suggested that these were GC precursors. Similarly, we found that the PE-specific CD38+ GL7+ B cells induced by PE injection expressed CCR6 and FAS (Fig. 4 A). However, PE-specific CD38+ GL7+ B cells bound low levels of PNA compared with genuine CD38− GL7+ GC B cells and did not express the GC fate-determining transcription factor Bcl-6 (Fig. 4 A). We tested the GC origin of CD38+ GL7+ B cells in radiation chimeras prepared with an equal mixture of Bcl6−/− and WT bone marrow cells. As reported by others (Dent et al., 1997; Fukuda et al., 1997; Toyama et al., 2002; Nurieva et al., 2009), Bcl-6 was required for the formation of CD38− GL7+ GC B cells (Fig. 3 B). In contrast, CD38+ GL7+ B cells formed equally well from Bcl6−/− and WT precursors (Fig. 4 C). Therefore, the PE-specific CD38+ GL7+ B cells did not appear to be committed to the GC pathway.
The early appearance of CD38+ GL7+ B cells after PE immunization raised the possibility that they were precursors of early memory cells and GC cells. To test this hypothesis, CD38+ GL7+ B cells from animals injected with PE in CFA 4 d previously were purified and transferred into recipient animals injected with PE in CFA at the same time as the donors (Fig. 5 A). CD38+ GL7− memory B cells emerged from CD38+ GL7+ donor B cells as early as day 2 after transfer (Fig. 5, B and C). GC B cells were also generated from the CD38+ GL7+ donor population, but not until day 4 after transfer (Fig. 5, B and C). Notably, CD38+ GL7+ B cells transferred into uninjected or CFA-injected recipients differentiated exclusively into memory B cells within 2 d after transfer (Fig. 5, B and C). Thus, CD38+ GL7+ B cells produced GC and memory B cells early in the primary response but only produced memory B cells when removed from antigen.
The results pointed to two pathways of memory cell formation. In one pathway, CD38+ GL7+ B cells differentiated directly into early memory cells without a GC cell intermediate. In the other, CD38+ GL7+ B cells differentiated into GC cells, some of which then became memory cells. We next aimed to determine the number of memory B cells that were generated from each pathway. This was done by counting memory B cells produced from WT or Bcl6−/− naive cells in the mixed chimeras described in Fig. 4. Because Bcl-6 is required for GC cell formation, any memory B cells that arise from Bcl6−/− naive B cells must be derived from the GC-independent pathway. IgM+ and swIg+ memory B cells were also identified in these experiments.
The number of IgM+ memory B cells generated by Bcl6−/− cells was comparable to the number generated from WT cells at all time points analyzed (Fig. 6, A and B). In contrast, the number of Bcl6−/− swIg+ memory B cells was similar to WT at day 6, but reduced threefold at day 10 and 30-fold at day 30 (Fig. 6 C). Thus, IgM+ and early swIg+ memory B cells were generated in a GC-independent fashion, presumably directly from CD38+ GL7+ precursors, whereas >95% of later swIg+ memory B cells were GC derived.
One potential caveat to these experiments was that cells that would have differentiated into GC cells were artificially shunted into the memory cell compartment when unable to express Bcl-6. We therefore aimed to distinguish GC-derived memory B cells from GC-independent memory B cells in WT animals. This was accomplished by using CD73 (ecto-5′-nucleotidase) expression to mark GC-derived memory B cells. CD73 is expressed by subsets of IgM+ and swIg+ memory B cells that have high levels of somatic hypermutation (Anderson et al., 2007; Tomayko et al., 2010) and expressed activation-induced cytidine deaminase (AID; Dogan et al., 2009), a molecule required for somatic hypermutation and Ig isotype switching. Given that somatic mutations are thought to occur predominantly in GC B cells, CD73 was a good candidate to mark GC-derived but not GC-independent memory B cells. This possibility was tested by analysis of WT plus Bcl6−/− mixed chimeras. Bcl6−/− B cells that were incapable of forming GC cells generated the same number of CD73− IgM+ memory B cells 31 d after immunization and only twofold less CD73− swIg+ memory cells than WT B cells (Fig. 7, A and B). In contrast, Bcl6−/− B cells produced fivefold fewer CD73+ IgM+ memory B cells and 100-fold fewer CD73+ swIg+ memory B cells (Fig. 7, A and B) than WT B cells at this time. Similarly, CD40 ligand blockade beginning at day 5 (Fig. 7 C) or day 17 (unpublished data), which reduced the number of GC B cells by 95% (Han et al., 1995; unpublished data), also resulted in a significant decrease in the number of CD73+ memory B cells present on day 30. Collectively, the data indicate that most GC-derived memory B cells express CD73, whereas most GC-independent memory B cells do not.
This conclusion was further supported by the kinetics of CD73− and CD73+ memory B cell formation in WT mice. As shown in Fig. 8 A, the number of PE-specific GC B cells peaked 14 d after injection of PE and CFA. Consistent with GC-independent differentiation, the vast majority of IgM+ memory B cells present at any time were CD73−, as were the swIg+ memory B cells that formed before the GC peak (Fig. 8, B and C). Consistent with GC-dependent differentiation, most swIg+ memory B cells present after the GC peak were CD73+ (Fig. 8 C). Furthermore, swIg+ CD73− memory B cells declined dramatically after day 10 (Fig. 8 D) in the same way that GC-independent swIg+Bcl6−/− memory B cells declined (Fig. 6). These results confirm the conclusion that IgM+ and early swIg+ memory B cells are generated in a GC-independent fashion, whereas most later swIg+ memory B cells are GC derived.
It was possible that the abundance of GC-independent CD73− IgM+ memory B cells was unique to priming with 15 µg PE in CFA. However, a 10-fold increase in the dose of injected PE to 150 µg induced the same number of CD73+ and CD73− memory B cells as injection of 15 µg (Fig. 8 E). A 10-fold reduction in the dose of injected PE to 1.5 µg resulted in a fivefold decrease in the total number of memory B cells, but the relative frequency of the CD73+ and CD73− subsets was largely unaffected (Fig. 8 E). Likewise, the use of alum as an adjuvant resulted in a decrease in the total number of memory B cells, but the relative frequencies of the CD73+ and CD73− subsets were similar to those induced by CFA (Fig. 8 E). These results indicate that large numbers of GC-independent IgM+ memory B cells are generated across a broad range of antigen doses and with two different adjuvants.
Earlier work demonstrated that CD40 signaling was required for antigen-driven B cell expansion and GC formation but, paradoxically, strong CD40 signaling with an agonistic CD40 antibody suppressed GC formation (Erickson et al., 2002). We used this antibody to test the possibility that T cell–derived CD40 signals were involved in the formation of GC-independent memory B cells. Consistent with prior work (Erickson et al., 2002), we found that administration of anti-CD40 at the time of injection of PE in CFA inhibited the formation of PE-specific GC B cells while slightly enhancing the formation of CD38+ GL7+ precursors and IgM+ and swIg+ memory B cells in WT mice (Fig. 9 A). The capacity of anti-CD40 to influence memory B cell formation was then tested in Tcra−/− T cell–deficient mice to determine if strong CD40 signaling was sufficient for the generation of GC-independent memory B cells. As reported previously (Pape et al., 2011), none of the activated phenotypes of PE-specific B cells were generated in Tcra−/− T cell–deficient mice injected with PE in CFA (Fig. 9 A). In contrast, PE-specific CD38+ GL7+ precursors and later IgM+ and swIg+ memory B cells were generated at or above WT levels in T cell–deficient mice injected with PE in CFA and anti-CD40, whereas GC B cells did not form at all (Fig. 9 A). Notably, the PE-specific swIg+ memory B cells found in anti-CD40–treated animals were CD73− (Fig. 9 B), providing additional evidence that they were derived from the GC-independent pathway. Thus, strong CD40 stimulation is required for CD38+ GL7+ B cell generation and sufficient for GC-independent memory B cell differentiation.
Our results show that GC-independent and GC-dependent memory B cells arise from developmentally plastic CD38+ GL7+ precursors. These precursors were capable of differentiating directly into memory B cells, mainly of the IgM+ variety, without passing through a GC cell intermediate stage. Alternatively, these precursors were capable of differentiating into GC B cells, some of which then became memory B cells, mainly of the swIg+ type. Therefore, our work confirmed earlier studies reporting that CD38+ GL7+ B cells could produce genuine GC B cells, but extended that work by showing that CD38+ GL7+ B cells could also directly generate GC-independent memory B cells.
Our results and the literature suggest the following scenario for the formation of CD38+ GL7+ B cells and their progeny. Previous work showed that naive B cells migrate to the border between the T and B cell areas after antigen binding and present antigen-derived peptide–MHCII complexes to helper T cells (Garside et al., 1998). This interaction results in CD40 signaling in the B cells causing them to proliferate (Garside et al., 1998). Our present work and that of Schwickert et al. (2011) suggests that CD38+ GL7+ B cells are early progeny of this proliferation at the T/B border. Our results further suggest that strong CD40 signals can cause CD38+ GL7+ B cells to differentiate directly into memory B cells without passing through a GC stage. Like Erickson et al. (2002), we observed that agonistic anti-CD40 treatment suppresses GC B cell formation in WT mice where T cell help is present. This suggests that strong CD40 signaling favors early memory cell formation by inhibiting GC B cell formation in a dominant fashion. Together, these results suggest that BCR and CD40 signals are required to generate CD38+ GL7+ B cells and that strong CD40 signaling directs these cells to become GC-independent memory B cells by preventing differentiation into GC B cells. Under normal circumstances, the B cells that receive these strong CD40 signals and become GC-independent memory B cells may be those that display large numbers of antigen-derived peptide–MHCII complexes, which induce large amounts of CD40 ligand on cognate helper T cells. In this model, CD38+ GL7+ B cells that receive weaker CD40 signals by interacting with a helper T cell displaying less CD40 ligand and providing other signals, such as IL-21, may differentiate into GC B cells.
CD38+ GL7+ B cells also converted into memory B cells when transferred into unimmunized mice. It is possible that some CD38+ GL7+ B cells received a strong CD40 signal and committed to the memory cell fate at the time of transfer, and simply completed this program in the antigen-free host. Alternatively, removal of BCR and CD40 stimulation may be a second pathway by which CD38+ GL7+ B cells become memory cells.
Validation of CD73 as a marker of GC-derived memory B cells allowed us to show that these memory cells arise 6 d after injection and are mostly swIg+. The abundance of swIg+ cells in the GC-dependent memory B cell population was expected because GC B cells express large amounts of AID. Accordingly, these memory cells have more somatic mutations and have undergone more affinity maturation than IgM+ memory cells (Pape et al., 2011). Blink et al. (2005) found that the frequency of IgG1+ memory B cells in the blood was similar at early and late times after immunization, whereas the fraction of the cells in the population with somatic hypermutations increased. This finding suggested that the IgG1+ memory cells found early in the response were short-lived and replaced by IgG1+ memory B cells coming from the GC at later time points. Although this is likely the case, the consistent decline of swIg+ memory B cells over long periods of time observed in our experiments (Pape et al., 2011) indicates that even the GC-selected swIg+ memory B cells have shorter half-lives than IgM+ memory B cells.
The result that most IgM+ memory B cells are GC independent explains our previous data showing that these cells exhibit a low level of somatic hypermutation (Pape et al., 2011). This result suggests that these cells did not express optimal amounts of AID, which is required for Ig isotype switching and somatic hypermutation. However, a population of IgM+ memory B cells containing BCR somatic mutations was marked in an AID reporter mouse described by Dogan et al. (2009). These IgM+ memory cells expressed CD73 (Dogan et al., 2009) and are likely the counterparts of the small GC-derived population of PE-specific CD73+ IgM+ memory B cells observed here.
In contrast, the data in humans indicates that most IgM+ memory B cells are GC derived (Klein et al., 1998; Seifert and Küppers, 2009). The difference between these conclusions may be the result from the use of CD27 to define memory B cells in humans. This definition may exclude GC-independent memory B cells because CD27 was adopted as a memory cell marker based on the fact that both CD27+ swIg+ and CD27+ IgM+ contained high levels of somatic hypermutation, whereas CD27− IgM+ cells lack mutations (Klein et al., 1998; Seifert and Küppers, 2009). Because nearly all individual CD27+ IgM+ B cells contain somatic mutations (Klein et al., 1998) and show other signs of passage through GC (Seifert and Küppers, 2009), it seems likely that GC-independent memory B cells reside within the CD27− IgM+ fraction. Consistent with this notion, ∼25% of swIg+ cells in human blood do not express CD27, are present, and show low levels of somatic hypermutation (Fecteau et al., 2006). Thus, the CD27− population of human B cells likely contains the products of this GC-independent pathway. CD27, which is up-regulated by GC B cells themselves (Jung et al., 2000), may simply be maintained by memory B cells after they leave the GC, whereas cells that bypass the GC never receive the stimulus to up-regulate CD27. In this way, CD27 expression in humans may be equivalent to CD73 expression in the mouse.
6–10-wk-old sex-matched mice were used for experiments. C57BL/6 (B6), Tcra−/−, B6.CD45.1 congenic (B6.SJL-Ptprca Pep3b/BoyJ), and 129Sv mice were purchased from The National Cancer Institute or The Jackson Laboratory and bred in house. Bcl6−/− mice on a mixed C57BL/6-129Sv background (Dent et al., 1997) were provided by A.L. Dent (Indiana University, Indianapolis, IN). All mice were maintained in a specific pathogen-free facility in accordance with University of Minnesota Institutional Animal Care and Use Committee and National Institutes of Health guidelines.
The spleen and inguinal, axillary, brachial, cervical, mesenteric, and periaortic LN were harvested into PBS for each mouse analyzed. In experiments examining the proliferation and differentiation of PE-specific cells, tissues were minced in collagenase D (Roche) and EDTA (Sigma-Aldrich), as previously described (Vremec et al., 1992; Itano et al., 2003), to increase the number of antibody-secreting cells recovered.
A single-cell suspension was prepared and resuspended to 0.2 ml in Fc block, consisting of culture supernatant containing Fc receptor antibody 2.4G2 (American Type Culture Collection), 2% rat serum (Serotec), and 0.1% sodium azide (Sigma-Aldrich). Each sample was incubated with 1 µg PE (Prozyme) for 30 min on ice or 0.5 µg allophycocyanin for 30 min at room temperature. Incubation with antigen was followed by a wash in 15 ml of ice-cold sorter buffer (DPBS with 2% fetal bovine serum [Thermo Fisher Scientific] and 0.1% sodium azide). PE- or allophycocyanin-stained cells were then resuspended to a volume of 0.2 ml of sorter buffer, mixed with 25–50 µl anti-PE– or anti-allophycocyanin–conjugated magnetic microbeads (Miltenyi Biotec) and incubated for 30 min on ice, followed by one wash with 15 ml of sorter buffer. The cells were then resuspended in 3 ml of sorter buffer and passed over a magnetized LS column (Miltenyi Biotec). The column was washed twice with 3 ml of sorter buffer and then removed from the magnetic field. Bound cells were eluted by pushing 5 ml of sorter buffer through the column with a plunger.
After centrifugation, cell pellets from the bound and flow through fractions were resuspended in 0.1 or 2 ml of sorter buffer, respectively, and 5 µl was removed from each sample for cell counting. The remaining cell suspensions were incubated with a cocktail of surface protein-specific antibodies for 25 min on ice and washed with sorter buffer. Antibodies used in various combinations were FITC-, AF647-, or Biotin-labeled GL7 (BD or eBioscience), AF700- or Pacific blue–labeled anti-CD38 (eBioscience or BioLegend), V500- or eF450-labeled anti-B220 (BD or eBioscience), AMCA-, PerCP-eF710–, or APC-labeled anti-IgM (Jackson ImmunoResearch Laboratories, Inc or eBioscience), PerCP-Cy5.5– or eF450-labeled anti-IgD (BioLegend or eBioscience), FITC- or PerCP-Cy5.5–labeled anti-CD45.1 (eBioscience), and APC-eF780–labeled anti-CD11c, anti-Thy1.2, anti-F4/80, and anti-Gr-1 (eBioscience). Because the IgM-AMCA antibody cross reacts with rat IgM, samples were first stained with IgM-AMCA, washed, and then preincubated with purified rat IgM (eBioscience) before the addition of GL7. In some experiments, cells were then stained with eF605NC-conjugated streptavidin (eBioscience) for 15 min on ice and washed with sorter buffer.
For analysis of isotype switching, cells were pelleted after surface staining and resuspended with 1 ml of 2% formaldehyde for 20 min on ice, followed by a wash with 2 ml of PBS. The cells were pelleted and resuspended in 1 ml of 0.5% saponin and incubated for 1 h with a cocktail of biotin-labeled anti-IgG1 (A85-1), IgG2c (5.7), IgG2b (R12-3), IgG3(R40-82; all from BD), IgA (RMA-1), and IgE (RME-1) antibodies (both from BioLegend), followed by Pacific blue–labeled streptavidin (Invitrogen). In some cases, isotype-switched cells were gated as cells that did not bind anti-IgM or anti-IgD.
For Bcl-6 analysis, cells were fixed with 0.25 ml Foxp3 Fixative (eBioscience) for 25 min on ice. Samples were washed with 3 ml of sorter buffer and incubated with AF488-labeled anti–Bcl-6 AF488 (BD) for 1 h.
Flow cytometry was performed on a 4-laser (355, 405, 488, and 633 nm) or 5-laser (355, 405, 488, 561, and 640 nm) LSR II device (BD) and analyzed with FlowJo software (Tree Star). Cell sorting was performed by the University of Minnesota Flow Cytometry Core using a 3-laser (407, 488, and 633 nm) FACSAria (BD). Fluorescent AccuCheck counting beads (Invitrogen) were used to calculate total numbers of live lymphocytes in the column bound and flow through suspensions as previously described (Moon et al., 2009). Samples collected after PE and CFA injection often had a significant number of PE-labeled B cells that were not retained by the column. When this occurred, these cells were included in the total number of cells.
Mice were injected s.c. with 50 µl CFA (Sigma-Aldrich) emulsion containing 15 µg of R-PE (Prozyme) or 7.5 µg allophycocyanin (Prozyme) except where noted. For CD40:CD40L blockade, mice were injected intraperitoneally with 0.5–1 mg anti-CD40L (Mr-1; BioXcell) every other day for 3 d beginning on either day 5 or 17. For CD40 stimulation, mice were injected intraperitoneally with 250 µg anti-CD40 (FGK4.5; BioXcell) every other day for beginning on the day of PE and CFA injection.
Purified naive B cells were prepared from spleen and LN of CD45.1+ mice using a B cell negative selection kit (Miltenyi Biotec). The B cells were washed in EHAA (Invitrogen), adjusted to a final concentration of 5 × 107 cells/ml in prewarmed EHAA, and incubated with 5 µM CFSE (Invitrogen) for 10 min at 37°C before they were injected intravenously into CD45.2 mice. Mice were injected with PE and CFA at least 1 d after adoptive transfer. Alternatively, cells were labeled with CellTrace violet (Invitrogen) according to the manufacturer’s instructions. To control for mouse-to-mouse and experiment-to-experiment differences in the number of donor cells that could be detected in recipient animals, the frequency of donor B cells was normalized to 1% for each donor-derived PE-specific B cell population with the formula c = (r/p) × 1%, where p is the percentage of donor-derived PE-negative B cells obtained from the column flow through, r is the absolute number of PE-specific B cells obtained experimentally, and c is the absolute number after the correction.
Bone marrow cells were prepared by crushing bones from Bcl6−/− and 129Sv × B6.CD45.1 F1 WT mice with a mortar and pestle in PBS. Bone marrow cells were labeled with anti-Thy1.2 and anti-NK1.1 (both from eBioscience), followed by incubation with rabbit complement (Cedarlane) for 30 min at 37°C to deplete T cells and NK cells. T cell– and NK cell–depleted Bcl6−/− and WT bone marrow cells were mixed 1:1 and 1–5 × 106 were injected into B6.CD45.1 recipient mice irradiated with 1,000 rad. The response of PE-specific cells in 129Sv × B6 CD45.1+ F1 mice was similar to that generated when control mixed chimeras were set up using Bcl6+/− or Bcl6+/+ littermate controls (unpublished data). Injections were done 8–10 wk after bone marrow transplantation. Variations in the absolute numbers of PE-specific B cells as a result of slight differences in chimerism were corrected to 50% for each donor-derived PE-specific B cell population with the formula, c = (r/p) × 50%, where p is the percentage of donor-derived PE-negative B cells obtained from the column flow through, r is the absolute number of PE-specific B cells obtained experimentally, and c is the absolute number after the correction.
LNs were harvested and frozen in OCT freezing medium (Sakura). 7-µm cryosections were dehydrated in acetone and blocked with 1% H2O2, culture supernatant containing 24G2 mAb plus 1% mouse and 1% rat serum, and avidin-biotin blocking reagents (Vector Laboratories). PE-binding cells were detected by incubating sections with PE followed by biotin-labeled anti-PE (produced by K. Pape), HRP-labeled streptavidin (PerkinElmer), and TSA-direct Cy3-tyramide (PerkinElmer). In some cases, the PE incubation was omitted as a negative control. GL7+ cells were detected with FITC-labeled anti-GL7 (eBioscience), followed by AF488-labeled anti-FITC (Invitrogen). T cell areas were detected with biotin-labeled anti-Thy1.2 (eBioscience), followed by AMCA-labeled streptavidin (Jackson ImmunoResearch Laboratories, Inc.). B cell follicles were detected with AF647-labeled anti-IgD (eBioscience). Images were captured with 10, 20, and 40× objective lenses on an automated upright microscope (DM5500B; Leica) and a digital camera (DFC340FX; Leica). Photoshop (Adobe) was used to process the images for display.
All p-values were determined using an unpaired two-tailed Student’s t test in Prism (GraphPad Software).
|AID||activation-induced cytidine deaminase|
We thank J. Walter and R. Speier for expert technical assistance, D. Mueller and M. Pepper for reviewing the manuscript, T. Martin, P. Champoux, and N. Shah for flow cytometry assistance, and all members of the Jenkins Laboratory for helpful discussions.
This work was supported by grants from the National Institutes of Health (R01 AI036914 and R37 AI027998 to M.K. Jenkins, and T32 CA009138 and F32 AI091033 to J.J. Taylor).
The authors have no conflicting financial interests.
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