Infection-induced plasmablasts are a nutrient sink that impairs humoral immunity to malaria

Abstract

Plasmodium parasite-specific antibodies are critical for protection against malaria, yet the development of long-lived and effective humoral immunity against Plasmodium takes many years and multiple rounds of infection and cure. Here we report that the rapid development of short-lived plasmablasts during experimental malaria unexpectedly hindered parasite control by impeding germinal center (GC) responses. Metabolic hyperactivity of plasmablasts resulted in nutrient deprivation of the GC reaction limiting the generation of memory B cell and long-lived plasma cell responses. Therapeutic administration of a single amino acid to experimentally infected mice was sufficient to overcome the metabolic constraints imposed by plasmablasts and enhanced parasite clearance and the formation of protective humoral immune memory responses. Thus, our studies not only challenge the current paradigm describing the role and function of blood-stage Plasmodium-induced plasmablasts, but also reveal new targets and strategies to improve anti-Plasmodium humoral immunity.

Introduction

Following either vaccination or microbial infection, humoral immunity generally consists of temporally and spatially layered B cell activation events. Early humoral responses are associated with extrafollicular B cells that proliferate and rapidly differentiate into short-lived antibody secreting cells (ASCs), also referred to as plasmablasts¹. T cell-dependent follicular responses take longer to develop and involve antigen-specific B cells forming a germinal center (GC) where they engage in sustained interactions with CD4⁺ T follicular helper cells (T_FH). GC B cells subsequently differentiate into either memory B cells (MBCs) or long-lived plasma cells (LLPCs) that secrete high-affinity, class-switched antibodies^{1, 2}. It is thought that extrafollicular, short-lived plasmablasts limit pathogen dissemination^{3, 4} until LLPC and MBC responses develop, which act to resolve the primary infection and mediate resistance to subsequent pathogen exposures⁵.

Plasmodium infections caused an estimated 219 million cases of malaria and resulted in approximately 435,000 deaths in 2017⁶. Both clinical and experimental studies identify Plasmodium-specific antibodies as critical for both limiting disease severity and promoting clearance of blood-stage parasites⁷. Although durable immunity to either P. vivax or P. falciparum has been reported in travelers and individuals from areas of relatively low transmission intensity^{8, 9, 10}, in regions of high P. falciparum transmission, parasite-specific LLPCs and MBCs are not efficiently induced and sterilizing immunity against blood-stage P. falciparum is seldom acquired, even following repeated infections^{11, 12}.

Multiple mechanisms have been postulated to explain the short-lived nature of Plasmodium-specific humoral immune responses, including preferential expansion of CXCR3⁺ (T_H1-like) T_FH cells¹³, regulatory T cells^{14, 15} and atypical MBCs^{16, 17, 18, 19}, as well as the dysregulation of chemokines and cytokines^{20, 21} and induction of immune checkpoints^{22, 23} that may delay or impair the acquisition of humoral immunity against malaria. Although these studies have identified numerous mechanisms that may contribute to the lack of durable immunity against malaria, our past studies showed that genetic manipulations that either expand or constrain the Plasmodium-specific GC response²⁴ are associated with substantially blunted or elevated plasmablast responses, respectively (Guthmiller and Butler, unpublished observations). These data raise the possibility that blood-stage Plasmodium infections may preferentially induce immunosuppressive plasmablast populations that reduce the development of GC B cell responses and the induction of long-lived humoral immunity. Herein, we used combinations of clinical trials and experimental rodent malaria models to define the dynamics of infection-induced plasmablast populations and interrogate their contribution to anti-Plasmodium immunity. Our data show that clinical and experimental blood-stage Plasmodium infection preferentially expands short-lived plasmablast populations and that during experimental malaria these cells may function as a metabolic sink that constrains GC-derived humoral immune reactions, thereby identifing a previously unknown mechanism by which Plasmodium parasites subvert host immunity.

Results

Plasmablasts dominate the response to Plasmodium infection

To examine the kinetics and magnitude of splenic ASC/plasmablast responses during experimental malaria, we infected wild-type C57BL/6 mice with Plasmodium yoelii (Py) strain 17XNL parasitized red blood cells (pRBCs). This infection is normally non-lethal to wild-type C57BL/6 mice and it mimics aspects of severe anemia and hyperparasitemia associated with P. falciparum infection of malaria-naïve individuals. We quantified activated and/or class-switched (IgD^neg) CD19⁺ B cells that expressed the adhesion and migratory factor CD138 (syndecan-1) (Extended Data Fig. 1a). Both splenic (Fig. 1a) and circulating (Extended Data Fig. 1b) CD138^hiIgD^neg plasmablast populations numerically peaked on day 10 post-infection (p.i.), underwent rapid contraction and returned to pre-infection numbers in the spleen by day 28 p.i. Notably, approximately 60–80% of all activated (IgD^neg) splenic B cells displayed characteristics of CD138^hi plasmablasts on day 10 p.i. By comparison, blood-stage Py infection-induced splenic GC (B220⁺GL7⁺CD95⁺) B cell responses slowly accumulated through day ~21 p.i. and persisted after parasite clearance (Fig. 1b), as previously described ²⁵. As expected, blood-stage Py infection-induced CD138^hi B cells uniformly expressed Blimp-1 (Fig. 1c), a transcriptional repressor encoded by Prdm1 that is essential for plasmablast development²⁶. CD138^hi plasmablast populations also secreted either IgM or IgG and at least a fraction of the cells reacted with Py-infected RBC lysate antigen (Fig. 1d,e and Extended Data Fig. 1c). Relative to CD138^loCD19^hi B cells, CD138^hi plasmablasts also retained intermediate expression of CD19 (Extended Data Fig. 1d), unlike LLPCs that fully down-regulate CD19²⁶. CD138^hi plasmablasts or their precursors incorporated 5-bromodeoxyuridine (BrdU) between days 6–10 p.i. (Extended Data Fig. 1e) and the cells exhibited higher forward scatter (Extended Data Fig. 1f), both of which are characteristics of proliferating/blasting cells. In agreement with the notion that these cells are actively engaged in antibody synthesis, CD138^hi plasmablasts exhibited extensive rough endoplasmic reticulum (Fig. 1f). At the peak of the response on day 10 p.i., ~40% of CD138^hi plasmablasts exhibited caspase-3 and −7 activation (Fig. 1g) and by day 21 p.i., the number of CD138^hi plasmablasts in the bone marrow was similar to that in naïve mice (Extended Data Fig. 1g), suggesting that their disappearance from the spleen and blood may be linked to apoptosis and was unlikely due to rapid migration of CD138^hi plasmablasts to the bone marrow.

Fig. 1. Preferential expansion of plasmablasts during experimental malaria.

a, Plots showing kinetics of splenic CD138^hiIgD^neg B cells, representative of 6 biologically independent experiments with similar results. b, Numbers of splenic plasmablasts (CD138^hiIgD^neg), GC B cells (GL7⁺Fas⁺) and kinetics of parasite burden (% of infected red blood cells) during Py infection. Data are means ± s.d. and representative of n = 3 biologically independent experiments with similar results using n = 5 (PB and GC B cells) and n = 4 mice (parasitemia). c, Blimp-1-eYFP expression among CD138^hiIgD^neg (green), CD138^loIgD^neg (blue) and CD138^loIgD^hi (red) cells on day 10 p.i. Data are representative of n = 2 independent experiments with n = 8 mice. d, Parasite-specific IgM and IgG antibody secreted by splenic CD138^hiIgD^neg plasmablasts isolated on day 10 p.i. Data are means ± s.e.m., pooled from 2 biologically independent experiments with n = 6 wells (media only) wells and n = 12 wells (CD138^hiIgD^neg). e, Numbers of parasite-specific antibody secreting CD138^hiIgD^neg plasmablasts isolated on day 10 p.i. Data are means ± s.e.m., pooled from n = 2 biologically independent experiments with n = 8 (IgG) and n = 11 mice (IgM). f, Transmission electron micrographs of indicated cells isolated on day 10 p.i. Data representative of n = 3 biologically independent experiments with similar results using n = 100 cells for each population and 1 mouse/experiment. Scale bar, 2 μm. Yellow arrows, rough endoplasmic reticulum. g, FLICA staining in CD138^hiIgD^neg plasmablasts (green) and naïve B cells (red) on day 10 p.i. Data representative of n = 2 biologically independent experiments similar results using n = 6 mice/time point. h, Confocal micrographs of day 10 p.i. spleen showing CD4 T cells (gray), total B cells (red), germinal center B cells (blue) and CD138^hi plasmablasts (green). Data representative of n = 2 biologically independent experiments using n = 3 mice. Scale bar, 300μm.

The spleen contains a heterogeneous population of B lymphocytes that includes follicular (FO, CD21^intCD23⁺) and marginal zone (MZ, CD21^hiCD23^neg) B cells (Extended Data Fig. 1h). Splenic CD138^hi plasmablasts are reported to differentiate from either FO or MZ B cells²⁷. We found that CD138^hi plasmablasts did not exhibit characteristics of FO B cells and only a minor proportion (~15%) exhibited characteristics of MZ B cells, whereas blood-stage Py infection-induced activated (CD138^loIgD^neg) B cells and the bulk of resting (CD138^loIgD^hi) B cells displayed characteristics of either FO or MZ B cells (Extended Data Fig. 1i). CD138^hi plasmablasts also did not express markers of GC B cells (GL-7⁺Fas⁺) (Extended Data Fig. 1j). In agreement with this surface phenotype, the majority of blood-stage Plasmodium infection-induced CD138^hi plasmablasts localized outside of B cell follicles (Fig. 1h). Together, these data support that blood-stage Plasmodium infection is associated with transient yet substantial accumulations of CD138^hiIgD^neg plasmablasts that localize outside of follicles.

CD138^hi plasmablasts constrain anti-Plasmodium humoral immunity

The significant expansion and accumulation of CD138^hi plasmablasts suggests they may play a critical role in mediating host protection against blood-stage Plasmodium infection. To test this hypothesis, we first transferred CD138^hi plasmablasts purified from Py-infected donors to Py-infected recipient mice 5 days before the peak of the endogenous CD138^hi plasmablast response in recipients (Extended Data Fig. 2a). Notably, transfer of CD138^hi plasmablasts resulted in higher parasite burdens (Fig. 2a), compared to recipients receiving either activated (CD138^loIgD^neg) B cells or PBS. Recipients of CD138^hi plasmablast also exhibited lower titers of parasite lysate-specific IgG2b on day 21 p.i. (day 16 post-transfer) (Fig. 2b). Next, we employed a genetic approach focused on Prdm1. We generated competitive mixed bone marrow chimeric mice in which we could conditionally and selectively delete Prdm1 from the B cell compartment (Extended Data Fig. 2b). Tamoxifen treatment of Py-infected Cre⁺ chimeric mice abrogated CD138^hi plasmablast responses (Fig. 2c) and enhanced parasite control (Fig. 2d). Genetic blockade of plasmablast development also resulted in 8 to 10-fold increases in number of GC B cells (Fig. 2e) and GC-T_FH-like cells (Fig. 2f and Extended Data Fig. 2c) and higher titers of merozoite surface protein 1 (MSP1₁₉)-specific serum IgG2b (Fig. 2g). Importantly, tamoxifen had no effect on parasite growth when administered to either Py-infected Cre^neg chimeric (not shown) or wild-type mice (Extended Data Fig. 2d) and inducible deletion of Prdm1 did not instead simply skew B cell differentiation towards the GC fate in Py-infected chimeric mice (Extended Data Fig. 2e,f).

Fig. 2. Blocking plasmablast development improves humoral immunity.

a,b, Py-infected mice were transferred either CD138^hiIgD^neg plasmablasts, CD138^loIgD^neg activated B cells or PBS. Kinetics of parasite burden (a) and anti-parasite IgG2b serum antibody endpoint titers (EPT) on day 21 p.i (b) in recipients. Data in a are means ± s.e.m pooled from n = 2 independent experiments with n = 7 (IgD^negCD138^hi) and n = 8 (IgD^negCD138^lo and PBS) mice analyzed by two-way ANOVA with Tukey’s multiple comparison test (DF = 14; F = 2.603). Data in b are means ± s.d. and representative of n = 2 biologically independent experiments with similar results using n = 4 mice/group. c-g, Rosa26-ERT2/Cre Prdm^fl/fl : μMT bone marrow chimeras infected with Py were either treated with vehicle (corn oil) or tamoxifen on days 4, 5 and 6 p.i. Plots showing abrogation of plasmablasts on day 10 p.i. (c) and kinetics of parasite burden (d). Data are means ± s.e.m, pooled from n = 2 independent experiments with n = 6 mice/group. e-g, Numbers of splenic GC B cells (e), GC-T_FH-like cells (f) and anti-Py serum antibody EPT (g) on day 21 p.i. Data are means ± s.e.m., pooled from n = 2 biologically independent experiments with n = 6 (corn oil) and n = 7 mice (tamoxifen). For d, data were analyzed using two-way ANOVA with Sidak’s multiple comparison test (DF= 9; F= 3.1). For b,e,f, and g, two-tailed Mann-Whitney tests were used for statistical analyses. Symbols in b, e-g represent individual mice.

Although elevated parasite-specific antibody titers and enhanced parasite control were somewhat unexpected in the absence of Blimp-1, previous studies showed that antigen-specific IgG secretion is only modestly reduced in splenic B cell subsets lacking Prdm1²⁸. However, early production of natural killer cell- and T_H1-derived IFN-γ can suppress Plasmodium replication early after blood-stage infection^{29, 30} and we observed 2-fold increases in Ly6C⁺CXCR3⁺IFN-γ⁺ T_H1-like cell responses in tamoxifen-treated, Py-infected Cre⁺ chimeric mice (Extended Data Fig. 2g). These data support that blood-stage Py infection-induced CD138^hi plasmablasts suppress GC responses and constrain anti-Plasmodium humoral immunity.

Deletion of plasmablasts improves humoral immunity

To confirm the effects of abrogating the CD138^hi plasmablast response without impacting GC-derived plasma cell responses, we generated CD138-DTR bone marrow chimeric mice in which CD138⁺ hematopoietic cells could be deleted using diphtheria toxin (DTx) (Extended Data Fig. 3a). Importantly, this approach deletes plasmablasts and plasma cells at the time of treatment, but allows the development of future LLPCs. DTx-mediated deletion of CD138^hi plasmablasts (Fig. 3a) in Py-infected chimeric mice resulted in decreased parasite burden (Fig. 3b), increases in both the number of GC B cells (Fig. 3c) and GC-T_FH-like cells (Fig. 3d), as well as elevated serum titers of MSP1₁₉-specific IgG (Fig. 3e) on day 21 p.i. Concomitant with the loss of CD138^hi plasmablasts, DTx-treatment transiently reduced the number of splenic ASCs on day 10 p.i. However, numbers of splenic ASC were elevated on days 15 and 21 p.i. in DTX-treated mice (Fig. 3f,g), perhaps as a result of GC-derived ASC formation. No differences in either parasite burden, GC B cells or GC-T_FH-like cells were observed when Py-infected wild-type mice were treated with DTx (Extended Data Fig. 3b–d). Thus, reduced parasite loads and elevated GC responses in DTx-treated CD138-DTR chimeric mice were a consequence of CD138^hi plasmablast deletion, and not due to any direct effect of DTx on parasite growth or immune cell activation.

Fig. 3. Deletion of plasmablasts enhances humoral immunity.

a-g, CD138-DTR bone marrow chimeras were infected with Py and treated with either vehicle (PBS) or diphtheria toxin (DTx) on days 5 and 7 p.i. Plots showing deletion of plasmablasts on day 10 p.i (a) and kinetics of parasite burden (b). Data are means ± s.e.m, pooled from n = 2 biologically independent experiments with n = 7 mice/group analyzed with a two-way ANOVA with Sidak’s multiple comparison test (DF = 6; F = 8.777). c, Numbers of splenic GC B cells. Data are means ± s.d. representative of n = 2 biologically independent experiments with similar results using n = 5 (PBS) and n = 4 mice (DTx). d, Numbers of splenic GC-T_FH-like cells. Data are means ± s.d. representative of n = 2 biologically independent experiments with similar results using n = 5 mice/group. e, Anti-MSP1₁₉ specific serum antibody EPT on day 21 p.i. Splenic plasmablast kinetics as detected by flow cytometry (f) and ELISPOT (g). Data in e-g are means ± s.e.m., pooled from n = 2 biologically independent experiments with n = 6 mice/group. Symbols in c-e represent individual mice. For panels c-g, data were analyzed using two-tailed Mann-Whitney.

In order to examine whether the improved parasite control in DTx-treated CD138-DTR chimeric mice was linked to enhanced GC responses, we distrupted CD4 T cell-mediated co-stimulation by adminstering CD40L blocking antibody (clone MR1) on days 8–11 p.i. Anti-CD40L treatment of DTx-treated mice reduced the frequency and numbers of GC B and GC-T_FH-like cells by 3 to 5-fold and fully abrogated parasite control (Extended Data Fig. 3e–g). Taken together, these cellular, biochemical and genetic manipulations support that blood-stage Py infection-induced CD138^hi plasmablasts suppress GC responses and contribute to increased parasite burden during the acute phase of experimental malaria.

CD138^hi plasmablasts are metabolically hyperactive

To gain insight into the potential mechanisms by which blood-stage Py-induced CD138^hi plasmablasts constrain GC responses, we performed RNA-seq analysis on splenic CD138^hi plasmablasts, as well as activated (CD138^loIgD^neg) and resting (CD138^loIgD^hi) B cell populations that are each present on day 10 p.i. (Fig. 4a). Principal component analysis (PCA) revealed that the three populations of B cells clustered distinctly from each other (Fig. 4b) with resting and activated B cells more similar to each other than CD138^hi plasmablasts (Extended Data Fig. 4a,b and Supplementary Table 1). Of the 3600 genes that were differentially expressed among the populations, multiple metabolism-related genes that play pivotal roles in the glycolytic and citric acid cycle pathways were distinctly expressed in CD138^hi plasmablasts, compared to either activated or resting B cells (Fig. 4c and Supplementary Table 2,3). CD138^hi plasmablasts also exhibited 5-fold higher basal respiration compared to the other two populations analyzed (Fig. 4d). Notably, our RNA-seq data also showed that CD138^hi plasmablasts exhibit gene signatures consistent with induction of the unfolded protein response pathway that is induced upon plasma cell formation^{26, 31} (Extended Data Fig. 4c and Supplementary Table 4), further supporting that blood-stage Py infection-induced CD138^hi plasmablasts are bona fide antibody secreting cells.

Fig. 4. Plasmablasts are metabolically hyperactive.

a, Gating strategy used for sorting plasmablasts and activated and resting B cell populations from Py-infected mice on day 10 p.i. that were used for bulk RNA-sequencing. b,c, Principal component analysis (PCA) depicting the clustering of transcriptomic data set from the three different B cell populations (b) and heat maps showing relative expression levels of different genes involved in glycolytic pathway (c, left) and citrate cycle pathway (c, right). d, Data comparing basal respiration of the three splenic B cell populations sort-purified from Py-infected mice on day 10 p.i. Data are means ± s.e.m. for n = 4 technical replicates, representative of n = 3 biologically independent experiments with similar results with n = 4 wells/cell type and analyzed by one-way ANOVA followed by Tukey’s multiple comparisons test. e,f, Heat map showing relative expression levels of various GLUT molecules (e) and network of various amino acid transporter pathways generated using Ingenuity Pathway Analysis (f). g, mRNA expression levels (relative to Hprt) of plasmablast specific genes (Prdm1, Xbp1s), B cell lineage gene (Pax5) and L-glutamine transporter molecules Slc1a4, Slc1a5, and Cd98 (Slc3a2 and Slc7a5). Data are means ± s.e.m. for n = 4 mice, representative of n = 2 biologically independent experiments with similar results using n = 2 technical replicates and analyzed by two-tailed Mann-Whitney. h, i, Frequency (h) and geometric mean fluorescence intensity (i) of CD98 expression on the indicated B cell populations isolated on day 10 p.i. Data are means ± s.d., representative of n = 2 biologically independent experiments with similar results using n = 4 mice and analyzed by one-way ANOVA. Symbols in b, d, g, h and i represent individual wells/mice. For panels a-c, e and f, n = 4 mice with data acquired from one experiment and analyzed by two-way ANOVA (FDR < 0.05 and fold change < −2 > 2).

We next sought to investigate factors associated with the increased metabolism of CD138^hi plasmablasts. B cell activation and proliferation and increases in biomass require an ample supply of biomolecules such as N, S, PO₄ and C and the acquisition of amino acids, especially L-glutamine (L-glut) ^{32, 33}. This requirement raised the possibility that substantial numbers of CD138^hi plasmablasts triggered by blood-stage Py infection may deplete local metabolic resources in the spleen. In support of this hypothesis, targeted analysis of our RNA-seq data set revealed that multiple amino acid and nutrient transporters were differentially expressed among the splenic B cell populations (Fig. 4e and Supplementary Table 5). Ingenuity Pathway Analysis (IPA) revealed broad activation of genes encoding solute carrier (SLC) transporters that are involved in amino acid acquisition, particularly L-glut (Fig. 4f). The activation of these pathways was also associated with CD138^hi plasmablast metabolic hyperactivity and expression of Blimp-1, which is known to promote the expression of amino acid transporters²⁸. We confirmed the upregulation of a set of L-glut SLCs, including mRNAs for Slc1a4 and Slc1a5, which correlated positively with Prdm1 and Xbp-1 and inversely with Pax5 mRNA expression (Fig. 4g). We also confirmed elevated mRNA and protein expression of Slc7a5 (CD98), another key SLC transporter that mediates L-glut uptake^{32, 33} (Fig. 4g–i). Together, these data support the hypothesis that metabolically hyperactive CD138^hi plasmablasts utilize SLC protein family members to increase the uptake of L-glut, which may in turn deplete key splenic metabolic resources required to sustain GC responses.

L-glutamine enhances anti-Plasmodium humoral immunity

Studies of Plasmodium-infected non-human primates and patients in malaria endemic areas revealed significant reductions in plasma L-glut concentrations during the acute phase of infection, which correlated with poorer outcomes and increased parasite burdens³⁴. Similarly, splenic L-glut concentrations were reduced in Py-infected mice (Extended Data Fig. 5a). Given their numerical overrepresentation and increased expression of machinery required to uptake L-glut, we hypothesized that blood-stage Py infection-induced CD138^hi plasmablasts impede GC reactions by acting as a nutrient sink, effectively incapacitating GC B and/or T_FH cells. To test this hypothesis, we supplemented the drinking water of Py-infected mice with L-glut (H₂O+L-glut) and monitored parasite growth and various immune parameters. Notably, mice receiving ad libitum L-glut exhibited 65% lower total parasite burden compared to mice on regular drinking water (Fig. 5a,b). There were no observable impacts on parasite control when the drinking water was supplemented with either the essential branched chain amino acid L-alanine or the non-essential neutral amino acid L-valine (Extended Data Fig. 5b,c), which like L-glut is transported by SLC1A5. Importantly, the protective effects of L-glut supplementation required the presence of CD4⁺ T cells (Fig. 5c), functional T_FH cells (Fig. 5d), and secreted antibody responses (Fig. 5e). Disruption of GC reactions via anti-CD40L also abrogated parasite control and GC B and T_FH cell responses in L-glut-treated mice (Extended Data Fig. 5d–f). Thus, enhanced parasite control in L-glut-treated mice was directly linked to improved GC reactions and humoral immunity, and not simply impacting upon the general physiology of either the host, host microbiome or the parasite itself.

Fig. 5. L-glutamine supplementation enhances germinal center responses.

a-n, Mice of the indicated genotypes were either left untreated (H₂O) or treated with L-glutamine supplemented water (H₂O + L-glut) starting on day 0 p.i. a,b, Kinetics of parasite burden (a) and area under curve as a measure of total parasite biomass (b). Data are means ± s.d., representative of n = 3 biologically independent experiments with similar results using n = 4 mice/group. Data in a were analyzed using a two-way ANOVA with Sidak’s multiple comparison test (DF = 6; F = 6.542). c, Kinetics of parasite burden in wild-type mice treated with either GK1.5 or rIgG on days 5 and 7 p.i. Data are means ± s.e.m., pooled from n = 2 biologically independent experiments with n = 6 (H₂O+L-glut+GK1.5, H₂O+GK1.5 and H₂O+rIgG) and n = 7 mice (H₂O+L-glut+rIgG). d, Kinetics of parasite burden in CD4-Cre x Bcl6^fl/fl mice. Data are means ± s.e.m., pooled from n = 2 biologically independent experiments with n = 7 mice/group. e, Kinetics of parasite burden in Aicda^−/−μS^−/− mice. Data are means ± s.e.m, pooled from n = 2 biologically independent experiments with n = 6 mice/group. f,g, Numbers of splenic GC B cells (f) and GC-T_FH-like cells (g) on day 12 p.i. in Py-infected mice. Data are means ± s.e.m, pooled from n = 2 biologically independent experiments with n = 6 mice/group. h,i, Anti-MSP1₁₉ IgG serum titers on days 12 and day 15 p.i. Data in h,i are means ± s.e.m, pooled from n = 2 biologically independent experiments with n = 6 (h), n = 9 (i, H₂O) or n = 8 mice mice/group (i, H₂O + L-glut). j-m, Confocal micrographs (j, scale bars, 500 μm), numbers of B cell follicles (k, n = 8, H₂O; n = 7 mice, H₂O + L-glut), number of GL7⁺ B cell follicles (l, n = 7 mice/group) and the surface area of B cell follicles per focal area (m, n = 58 foci, H₂O; n = 78 foci, H₂O+L-glut) in the spleens of mice on day 12 p.i. Data in k-m are means ± s.e.m, pooled from n = 2 biologically independent experiments. n,o, Oxygen consumption rates (n) and basal respiration (o, minutes 0–20) of plasmablasts and activated B cells isolated on day 10 p.i. Data in n,o are means ± s.e.m., representative of n = 2 biologically independent experiments with similar results using n = 5 (PB, H₂O; activated B cells H₂O+L-glut) and n = 6 (activated B cells, H₂O; PB, H₂O+L-glut) technical replicates using 2.5 × 10⁵ cells/well sorted from n = 3 mice/group. Symbols in b, f, g, h, i, k and l represent individual mice. Symbols in m and o represent technical replicates. Data in m were analyzed using a two-tailed unpaired t test (t = 2.505, df = 134). Data in f, g, h, i, k, l and o were analyzed with two-tailed Mann-Whitney.

Consistent with the requirements for secreted antibody and T_FH cells for enhanced parasite control following L-glut treatment, we observed higher magnitude GC B cell responses that appeared with accelerated kinetics (Fig. 5f and Extended Data Fig. 5g), as well as elevated numbers of class switched GC B cells in the spleen as early as day 12 p.i. (Extended Data Fig. 5h). While the numbers of CD138^hi plasmablasts were not significantly affected (Extended Data Fig. 5i), L-glut supplementation also increased the numbers of GC-T_FH-like cells by day 12 p.i. (Fig. 5g and Extended Data Fig. 5j), but did not alter Bcl-6 expression within these cells (Extended Data Fig. 5k). The accelerated and enhanced GC B cell and T_FH cell responses also translated into higher serum titers of MSP1₁₉-specific IgG on both days 12 and 15 p.i. (Fig. 5h,i). Histological analyses confirmed L-glut treatment enhanced the retention of splenic/follicular architecture and elevated the number and size of GCs (Fig. 5j–l). L-glut supplementation did not enhance either T_H1-like cell responses or the activation status of splenic dendritic cells (Extended Data Fig. 5l,m), although these data do not formally exclude a potential role for their contribution to enhanced parasite control.

To investigate whether L-glut supplementation altered the metabolic status of splenic B cells, we sorted CD138^hi plasmablasts and activated (CD138^loIgD^neg) B cells, which includes both activated FO and MZ B cells, from spleens of Py-infected mice receiving either regular or L-glut supplemented water and measured oxygen consumption rates (OCR) (Fig. 5m). L-glut supplementation increased the basal OCR of activated B cells, but not CD138^hi plasmablasts (Fig. 5n). Notably, L-glut could enhance parasite control when administered as late as day 6 p.i. (Extended Data Fig. 5n,o), but the protective effects were not observed when L-glut administration was initiated after the peak numerical expansion of plasmablasts (day 10 p.i.) (Extended Data Fig. 5p,q). Collectively, these data are consistent with the notion that CD138^hi plasmablasts, by virtue of their metabolic hyperactivity and their potential to uptake L-glut, transiently impair the metabolic and optimal functions of other splenic B cell populations. Thus, L-glut, when delivered either prophylactically or therapeutically, may relieve GC B and T_FH cells from nutrient deprivation to enhance their numbers and functions.

Plasmablast deletion and L-glutamine are functionally redundant

The deletion of plasmablasts and L-glut treatment both reduce parasitemia, increase the GC response and boost the activation of B cells as measured by OCR. To test whether these phenotypes are connected, and determine whether CD138^hi plasmablasts deletion and L-glut administration are functionally overlapping, we administered L-glut to DTx-treated CD138-DTR chimeric mice (Extended Data Fig. 6). As expected, both L-glut and DTx-treatment independently enhanced parasite control (Fig. 6a) and elevated the number of GC B cells (Fig. 6b) and GC-T_FH-like cells (Fig. 6c). However, these effects were not further enhanced when L-glut and DTx were combined (Fig. 6a–c). Furthermore, the metabolic activity of activated splenic B cells was elevated 8 to 12-fold in mice treated with either L-glut or DTx, yet the basal oxygen consumption was only minimally enhanced (~10%) when these treatments were combined (Fig. 6d). Taken together, these data suggest that CD138^hi plasmablast deletion and L-glut supplementation are functionally redundant, which additionally supports the model that CD138^hi plasmablasts may serve as a key glutamine sink during blood-stage Plasmodium infection.

Fig 6. Plasmablast deletion and L-glutamine are functionally redundant.

a-e, Py-infected CD138-DTR bone marrow chimeric mice were either left untreated (H₂O) or treated with L-glutamine supplemented water (H₂O + L-glut) starting on day 0 p.i. Mice were subsequently treated with either vehicle (PBS) or diphtheria toxin (DTx) on days 5 and 7 p.i. Kinetics of parasite burden (a) and numbers of splenic GC B cells (b) and GC-T_FH-like cells (c) on day 21 p.i. Data are mean ± s.e.m, pooled from 2 biologically independent experiments with n = 6 mice/group. Oxygen consumption rates (OCR) of activated B cells isolated from indicated groups on day 10 p.i. (d) and summary graph of basal respiration (e, minutes 0–20) among treatment groups. Data are means ± s.e.m., representative of n = 2 biologically independent experiments with similar results using n = 4 (H₂O+DTx and H₂O+L-glut+DTx) and n = 6 technical replicates (H₂O+PBS and H₂O+L-glut+PBS) with 2.5 × 10⁵ – 1 × 10⁶ cells/well sorted from n = 4 mice per group. Symbols in b and c represent individual mice. Symbols in e represent technical replicates. Data were analyzed with either a two-way ANOVA with Tukey post hoc test (a, DF = 18; F = 8.789) or two-tailed Mann Whitney (b-d).

Plasmablast deletion and L-glutamine improve immune memory

GC responses result in the production of LLPCs and MBCs that mediate protection against pathogen re-infection⁵. Accelerated and higher magnitude T_FH and GC reactions in DTx- and L-glut-treated mice are thus predicted to translate into increased numbers of MBCs, LLPCs and heightened resistance to a heterologous challenge with a lethal species of Plasmodium parasite, P. berghei-ANKA (PbA). In support of this notion, kinetic analyses revealed higher frequencies and numbers of (CCR6⁺CD38⁺)³⁵ MBCs in both DTx- (Fig. 7a) and L-glut-treated (Fig. 7d) mice between days 10 and 60 p.i. DTx- and L-glut-treated mice also exhibited elevated LLPC responses, whether these were measured using functional ELISPOT assays (Fig. 7b,e) or flow cytometry (Extended Data Fig. 7a,b). Mice treated with either DTx (Fig. 7c) or L-glut (Fig. 7f) during a primary Py infection were also more resistant to lethal PbA challenge, compared to their control counterparts. Of note, radiation chimeras are more resistant to lethal PbA challenge, which may explain the extended survival among both PBS- and DTx-treated chimeric mice, relative to the H₂O- and H₂O+L-glut-treated mice. Finally, we observed that MBC (Extended Data Fig. 7c) and LLPC (Extended Data Fig. 7d) responses were not enhanced when L-glut is adminstered from days 16–21 p.i., which is consistent with the therapeutic window during which L-glut functions to enhance parasite control (days 6–10 p.i.). Thus, the mechanisms by which L-glut promotes MBC and LLPC formation are likely linked to the enhanced function of the GC reaction and not strictly connected to enhancements in the post-GC survival of these cell subsets. Collectively, these data show that either CD138^hi plasmablast deletion or therapeutic administration of L-glut during an established blood-stage Plasmodium infection can be sufficient to accelerate the formation and increase the magnitude of GC reactions, which are further associated with enhancements in MBC, LLPC and protective immune memory responses.

Fig 7. Plasmablast deletion and L-glutamine enhance humoral immune memory.

a-c, Py-infected CD138-DTR bone marrow chimeras were treated with vehicle (PBS) or diphtheria toxin (DTx) on days 5 and 7 p.i. Kinetics of splenic memory B cells (a) and bone marrow antibody-secreting cells (b). Data in a,b are means ± s.e.m., pooled from n = 2 biologically independent experiments with n = 4 (day 60) and n = 6 mice/group (days 10, 15 and 21). c, Survival of mice challenged with Pb-Anka 30 days after an initial Py infection. Data are pooled from 2 biologically independent experiments with n = 7 (DTx) and n = 8 mice (PBS). d-f, Py-infected wild-type mice were either left untreated (H₂O) or treated with L-glutamine supplemented water (H₂O + L-glut) starting on day 0 p.i. d, Kinetics of splenic memory B cell responses. e, Kinetics of bone marrow antibody-secreting cells. Data in d,e are means ± s.e.m., pooled from n = 2 biologically independent experiments with n = 6 mice/group. f, Survival of mice challenged with Pb-Anka 30 days after an initial Py infection. Data are pooled from n = 2 independent experiments with n = 10 mice/group. Data in a, b, d, and e, were analyzed with two-tailed Mann Whitney. Data in c and f were analyzed with Mantel-Cox.

Robust plasmablast expansions during acute human malaria

To identify potential parallels between CD138^hi plasmablast inductions in mice and plasmablast expansions during acute human malaria, we evaluated peripheral B cell responses in forty humans in P. falciparum blood-stage volunteer infection studies (VIS). Cohorts of malaria-naïve subjects were challenged with P. falciparum (Pf)-infected RBCs and blood parasite burdens were monitored by qPCR at regular intervals until the end of the study (EOS) on day 27–36 p.i. (Extended Data Fig. 8). Subjects were treated with a schizonticidal drug when the infection reached ~20,000 parasites/mL, at day 8 p.i. Importantly, acute blood-stage P. falciparum infection resulted in transient yet substantial increases in the frequencies of CD19⁺CD3⁻CD27⁺CD38⁺ plasmablasts by day 14/15 p.i, with some subjects exhibiting plasmablast responses that comprised greater than 15% of their entire peripheral B cell pool (Fig. 8a). Notably, the magnitude of plasmablast expansion was positively correlated with total parasite biomass (Fig. 8b). These clinical data show that plasmablast responses are robustly induced in malaria-naïve humans at their first exposure to P. falciparum in a way similar to experimental murine models of malaria.

Fig 8. Positive correlation between parasite burden and plasmablasts in human malaria.

a, Plots (left panel, gated on CD19⁺CD3⁻ cells) and summary graph (right panel) showing the kinetics of plasmablasts in the peripheral blood of volunteers drawn on the indicated days during the course of the study. Boxplots are median ± IQR, whiskersare data range to 1.5 × IQR analyzed by two-sided Wilcoxon matched-pairs signed rank tests. b, Correlation graph showing the relationship between parasite burden on day 15 (area under curve, AUC) and the increase in plasmablasts numbers from day 0 to day 15 (delta PB-day 15). Data were analyzed by two-tailed Spearmans rho. Data in a,b derive from n = 36 men and n = 4 women from 4 studies across 6 independent cohorts.

Together, our observations in P. falciparum-infected humans, in combination with our rodent data, support the hypothesis that in malaria-naïve hosts the initial B cell activation events are numerically dominated by extrafollicular plasmablasts/CD138^hi B cells. Futhermore, our cellular, genetic and biochemical approaches support that plasmablasts functionally constrain germinal center responses and limit the induction of LLPC and MBC populations by acting as a metabolic sink that limits L-glut availability during experimental malaria.

Discussion

Rapidly forming, short-lived extrafollicular plasmablasts play complex roles in humoral immunity and host protection. Indeed, it is widely accepted that plasmablasts can provide an early source of protective antibody during bacterial infections^{36, 37}. Similar to LLPCs, short-lived plasmablasts express Blimp-1 and are equipped with the machinery to secrete antibodies¹. However, there are also data suggesting that plasmablasts may either inefficiently prime or directly inhibit T_FH cell activation and function^{38, 39, 40}, which may limit autoreactivity and tune the selection of B cell clones expressing the highest affinity receptors. While our data do not exclude the possibility that blood-stage Plasmodium infection-induced plasmablasts directly impair T_FH cell responses, our results show that either abrogation of plasmablast differentiation or deletion of plasmablasts during an established experimental Plasmodium infection resulted in enhanced clearance of the parasite, which was associated with 10-fold increases in the magnitude of the GC response. Our observations in mice are further supported by our P. falciparum VIS trials where substantial plasmablast expansions occured and were positively correlated with parasite burdens. Distinct from previous work showing immunosuppressive roles for either plasmablasts or plasma cells^{38, 39} our data reveal CD138^hi plasmablast populations comprise the dominant proportion of the total activated B cell pool following blood-stage Plasmodium infections. Thus, their overrepresentation may be a cardinal feature of blood-stage Plasmodium infections and potentially other infections of the blood that are associated with systemic inflammation, eryptosis, hemolysis, anemia and impairments in durable humoral immunity.

Plasmablast numbers have stood as a surrogate for protective immunity⁴¹. However, our assays revealed that few (~1%) plasmablasts express receptors that detectably interact with parasite antigens and that plasmablasts constrain rather than promote humoral immunity. Our efforts to identify potential mechanisms by which CD138^hi plasmblasts constrain GC-dependent MBC and LLPC formation revealed links to their metabolism. From a cell biological perspective, Plasmodium-infection induced plasmablasts resemble a transient plasmablastic lymphoma similar to diffuse large B cell lymphoma (DLBCL) characterized by downregulation of tumor suppressor genes and upregulation of genes that promote tumorigenesis. Moreover, tumor cells^{42, 43} and plasmablasts express an array of SLC molecules, likely to help meet the metabolic demands of their high rates of proliferation and increases in cellular biomass. It has also been reported that cancer cells are ‘addicted’ to glutamine and are capable of acting as a metabolic ‘sink’⁴⁴. Thus, we hypothesized that the large numbers and increased metabolic demands of plasmablasts together with their high expression of SLC molecules may cause energetic and metabolic shortfalls for other effector B cells in the spleen, which may in turn functionally incapacitate and/or delay the development of GC response. Consistent with this hypothesis, our studies show that supplementing the drinking water of Py-infected mice with L-glut could relieve an apparent plasmablast-mediated state of nutrient deprivation and elevate GC, MBC and LLPC responses. Our kinetic studies revealed a critical window during which L-glut supplementation can augment GC-dependent humoral immunity, which temporally overlaps with the expansion and maximal accumulation of Plasmodium blood-stage infection-induced plasmablasts. Thus, although both plasmablasts and GC B cells may exhibit similar metabolic requirements, the over-representation of plasmasblasts likely deprives GC B cells of critical nutrients required for their development and function. Future studies will be required to determine whether plasmablast deletion and associated changes in metabolic fitness of GC B cells also impact either B cell antigen receptor affinity maturation or epigenetic programming of MBCs and LLPCs. Although ¹³C-L-glutamine tracing studies designed to show that plasmablasts sink glutamine in vivo are warranted, these studies are confounded by the time required for tissue processing and cell sorting. Nevertheless, the composite of data support the model that plasmablasts serve as a key glutamine sink during blood-stage Plasmodium infection and the hypothesis that alternative, metabolism-based strategies may have clinically relevant applications for malaria.

Previous studies reported that dietary supplementation of L-arginine enhanced T cell responses in rodents during lethal Plasmodium infection⁴⁵ and that inhibiting glutamine metabolism with 6-diazo-5-oxo-L-norleucine (DON) improved survival and prevented the onset of experimental cerebral malaria (ECM) in mice challenged with Pb-ANKA⁴⁶. No mechanisms were identified in the L-arg study and the latter report primarily attributed the effects of DON to inhibition of CD8⁺ T cell degranulation, a key function that drives the onset of ECM. During experimental Plasmodium yoelii and Pb-ANKA infections truncated with anti-blood-stage drugs, neither of which cause CD8⁺ T cell-mediated immunopathology and ECM, CD8⁺ T cells were robustly activated²² and contribute to host protection⁴⁷. Thus, our data do not exclude the possibility that an enhanced parasite-specific CD8 T cell response also contributes to the improvements in host resistance to Plasmodium during L-glut supplementation. We predict that strategies to specifically inhibit L-glut uptake by plasmablasts would yield results similar to those we observed when we either abrogated plasmablast development or deleted these cells using genetic approaches. However, at present we know of no way to block either glutamine uptake or glutaminolysis specifically in plasmablasts. Nevertheless, our data and the experiments with L-arg and DON during experimental malaria highlight critical roles for immune cell metabolism and warrant the further exploration of strategies to modulate these cell biological processes in specific cell types.

In summary, our data support the model that during blood-stage Plasmodium infection, B cell differentiation is biased towards metabolically hyperactive, short-lived plasmablast responses that by their sheer numbers constrain GC reactions, likely due to glutamine deprivation. The preferential induction of extrafollicular, immunosuppressive plasmablasts represents an additional mechanism by which Plasmodium parasites subvert host protective immunity. Thus, the identification of an expansion of immuno-inhibitory plasmablasts during Plasmodium infection represents a conceptual shift with implications for either future immune- or metabolism-based strategies designed to limit plasmablast expansions, which may ultimately contribute to the development of durable humoral immunity against malaria.

Methods

Volunteer infection studies

P. falciparum blood-stage Volunteer infection trials (VIS), inoculum preparation, volunteer recruitment, infection, monitoring and treatment were performed as previously described⁴⁸. In brief, healthy malaria-naive individuals (n = 36 men, n = 4 women) underwent induced blood-stage malaria inoculation with 2800 viable P. falciparum 3D7-parasitized RBCs, and peripheral parasitemia was measured at least daily by qPCR as described previously⁴⁹. Participants were treated with antimalarial drugs at day 8 of infection. Blood samples from 40 volunteers (from 4 studies across 6 independent cohorts) were collected prior to infection (day 0), at peak infection (day 8) and 14 or 15 and 27–36 days (end of study, EOS) after inoculation (in analyses these time points are grouped as 0, 8, 14/15 and EOS). Plasma was collected from lithium heparin whole-blood samples according to standard procedures, snap frozen in dry ice and stored at −70°C. B-cells were analyzed from fresh whole blood at time of collection. All studies were registered with US NIH ClinicalTrails.gov (NCT02867059, NCT02783833, NCT02431637⁵⁰, NCT02431650⁵⁰). Participants were healthy adults 18 and 55 years with no prior exposure to malaria or residence in malaria-endemic regions. Area under the curve (AUC) were calculated using the trapezoidal method on serial log₁₀ transformed parasites/mL data from 4 days p.i. to each of the three defined timepoints (8, 14/15, and EOS similar to previously described⁵¹. Equation 1 below describes the calculation, with being each time point sampled, being the log₁₀ parasites/mL at that time, and being either 8 p.i., 14/15 p.i., or EOS. Samples where parasitaemia was not detected were substituted with 0 on the log₁₀ scale. The samples collected between the 4 defined timepoints (ranging from daily to twice daily before treatment, ranging from daily to every 2 h after treatment, and ranging from every four days to daily between timepoint 14/15 and EOS) were used in the calculation of AUC but not in any other analyses.

Study approval

Written informed consent was obtained from all participants. Ethics approval for VIS and the use of human samples was obtained from the Human Research and Ethics Committee of the QIMR-Berghofer Institute of Medical Research and Alfred Human Research and Ethics Committee for the Burnet Institute.

Animals, infections and parasitemia quantification

The University of Iowa IACUC approved all experiments. C57BL/6 WT (CD45.2 and CD45.1), Blimp-1eYFP (JAX stock #008828), μMT (JAX stock 002288) and Rosa26-ERT2/Cre (JAX stock 008463) mice were purchased from Jackson Laboratories. Aicda^−/−μs^−/− mice were a gift from F. Lund (UAB). CD138-DTR mice were generated via CRISPR/Cas9 editing at the U of Iowa genome editing facility. Male and female mice were used in all experiments, sex-matched only for adoptive transfers and generating chimeras. Plasmodium yoelli (clone 17XNL, obtained from MR4, ATCC) and Plasmodium berghei (clone ANKA, obtained from MR4, ATCC) stocks were generated by single passage in NIH Swiss Webster mice. Infections in experimental mice were initiated by a serial transfer (i.v.) of 1 × 10⁶ parasitized red blood cells (pRBCs) derived from a single donor C57BL/6 mouse. In some experiments, Py-infected mice were treated (i.p.) daily (days 8–11 p.i.) with 500 μg of either anti-CD40L (clone MR1) or Armenian Hamster IgG. CD4 T cell depletion was achieved by administering (i.p.) 200 μg of anti-CD4 antibody (clone GK1.5, BioXcell) on days 5 and 7 p.i. Parasitemia was measured using flow cytometry and is also depicted as area under the curve (AUC), which is a composition of parasite growth, peak burden and clearance kinetics^52,53.

CD138^hi adoptive transfers

Splenic CD138^hi B cells were enriched on day 5 p.i. using anti-CD138-APC (clone 281–2, BioLegend) and anti-APC magnetic beads (Miltenyi). CD19⁺CD138^hiIgD^neg plasmablasts and CD19⁺CD138^loIgD^neg activated B cells were sort purified. 1–2 × 10⁶ cells were transferred i.v. to mice on day 7 p.i. Mice that did not receive cells were given 200 μL of PBS i.v. on day 7. Sera and spleens were harvested from recipients on day 21 p.i. (day 14 post-transfer). Parasitemia was monitored every 2–3 days p.i.

Electron Microscopy

Electron microscopy was performed by the Central Microscopy Research Facility personnel at the University of Iowa. Images were captured on JEOL JEM 1230.

Confocal Imaging

After harvest, spleens were passed through a sucrose gradient (10% for 1 h, 20% for 2 h, 30% for 3 h) and flash frozen in Tissue Freezing Medium (General Data TFM-5) using a Gentle Jane Snap Freezer. 10 μm sections were cut and dried for 45 min in a 37 °C dry incubator. The sections were soaked in ice-cold Zinc Formalin Fixative (Sigma) for 15 min at −20°C then washed in 1× PBS (3 min/ wash). Sections were blocked with 1% BSA in 1× PBS for 2 h at 25 °C. After a 5-min wash in 1× PBS, sections were stained with the primary antibodies (in 1% BSA in 1× PBS) for 24 h at 4 °C. Sections were washed in 1× PBS (3 min/ wash) then mounted using hard set mounting medium for fluorescence (VECTASHIELD H-1400). Sections were stained with B220-AF488 (5 μg/ml; clone RA3–6B2, eBioscience), CD4-AF594 (10 μg/ml; clone GK1.5, BioLegend). GL7-AF647 (6.67 μg/ml; BD Pharmingen), and CD138-BV421 (1.67 μg/ml; clone 281–2, BioLegend). Imaging was done using a Zeiss LSM710 confocal microscope and processed using IMARIS x64 software (version 9.2.1).

Bone marrow chimeras

For generation of Rosa26-ERT2/Cre Prdm1^fl/fl : μMT chimeras, WT recipient (CD45.1) mice were irradiated with 475 rads twice separated by 4 h. Bone marrow cells from Rosa26-ERT2/Cre Prdm1^fl/fl (CD45.2) and μMT (CD45.1) were mixed 1:9 and 1 × 10⁷ cells were injected i.v. Mice were maintained on Uniprim diet (Envigo) for 2–3 weeks. Chimerism was assessed at 6 weeks and mice were infected with 10⁶ Py parasitized RBCs by 8 weeks. On days 5 and 7 post infection mice were either treated orally using a gavage needle, with 100 μL tamoxifen (4 mg/mouse) or corn oil. Depletion of plasmablasts was assessed on day 10.

For generation of CD138-DTR chimeras, WT (CD45.2) mice were irradiated with 475 rads twice separated by 4 h. 1 × 10⁷ cells bone marrow cells from CD138-DTR mice were injected i.v. Mice were maintained on Uniprim diet (Envigo) for 2–3 weeks. Chimerism was assessed at 6 weeks and mice were infected with 10⁶ Py parasitized RBCs. On days 5 and 7 post infection mice were treated i.p. with either diphtheria toxin or PBS intraperitonially. Depletion of plasmablasts was confirmed on day 10 p.i. For Rosa26-ERT2/Cre Prdm1^fl/fl: μMT : WT chimeras, bone marrow cells from Rosa26-ERT2/Cre Prdm1^fl/fl (CD45.2), μMT (CD45.1), WT (CD45.1) were mixed at 1:8:1 and 10⁷ cells were injected i.v into Rag1^−/− mice irradiated with 475 rads. Mice were maintained on Uniprim diet as above. Chimerism assessements, infections and tamoxifen treatments were as described above.

Tamoxifen and diphtheria toxin preparation and treatment

1 g of dessicated Tamoxifen (Sigma T5648) was dissolved in 5 mL of 200 proof ethanol, mixed with 20 mL of corn oil and stored at −20°C. On days 4, 5, and 6 post Py infection mice were administered 100 μL (4 mg/ mouse/dose) of the Tamoxifen corn oil mixture via oral gavage. 1 mg of lyophilized DTx (Sigma D0564) was resuspended in 3 mL of sterile PBS to achieve a concentration of 0.33 mg/mL. Mice were treated i.p. with 250 ng of DTx on the indicated days.

RNA Seq and GSEA

The three different B cell populations (resting B cells, activated B cells and plasmablasts) were flow-sorted from 4 Py-infected mice on day 10 p.i and RNA was extracted using NucleoSpin RNA kit (Takara Bio USA Inc.) according the manufacturer’s protocol. RNA sample integrity and quantity were determined using Tape Station Bioanalyzer (Agilent), with all samples showing RNA integrity numbers > 8. Twenty ng of total RNA was used for each library. Strand-specific RNA-Seq library was created using Illumina library creation protocol. The indexed libraries were pooled and sequenced using an Illumina NextSeq 550 sequencer using paired-end chemistry with 50 base pair (bp) read length Gene Expression Omnibus record: GSE134548. The quality of sequence reads was assessed using FastQC (http://www.bioinformatics.babraham.ac.uk/projects/fastqc/) and were aligned using STAR aligner⁵⁴ to the mouse genome version mm10 and the corresponding transcriptome. Following read alignment, gene expression profiles were computed using featureCounts⁵⁵. Next, differentially expressed genes were identified using Partek GS software and genes with significant changes were filtered using adjusted P-value of 0.05 as threshold. Visualization of differentially expressed genes represented as heat maps were generated using Partek GS software. Further, Ingenuity Pathway Analysis software (Qiagen Bioinformatics) was used to identify the underlying molecular pathways and interaction networks that involved the differentially expressed genes.

Quantitative Real Time PCR and Primers

The three different B cell populations (resting B cells, activated B cells and plasmablasts) were flow-sorted from 4 Py-infected mice on day 10 p.i. and RNA was extracted using NucleoSpin RNA kit (Takara Bio USA Inc.) according the manufacturer’s protocol. Two micrograms of RNA was used for cDNA synthesis. One microliter cDNA was added to 19 μL of PCR mixture containing 2X PowerUp SYBR Green Master Mix and 0.2 μM of forward or reverse primers. Amplification was performed in a QuantStudio3 thermocycler (Appiled Biosystems). Genes and forward and reverse primers are shown in Supplementary Table 6. Cycle threshold (Ct) values were normalized to those of the housekeeping gene hypoxanthine phosphoribosyltranferase (Hprt) by the following equation: ΔCt = Ct_{(gene of interest)} − Ct_(HPRT). All results are shown as a ration of HPRT calculated as 2^−(ΔCt).

ELISPOT

White polystyrene plates (Nunc Maxisorp) were coated with 0.5 μg/ml of either recombinant MSP1₁₉ or parasite infected red blood cell lysate. Plates were washed with PBS and blocked for at least 2 h with PBS/2.5% BSA/5% Goat Serum. Bone marrow cells or CD19⁺CD138⁺IgD^neg B cells sort-purified from Py-infected mice were used. Serial dilutions of cells in supplemented IMDM were added to each well for 20 h at 37 °C with 5% CO₂. Following extensive washes with PBS/0.05% Tween 20, HRP-conjugated goat anti-mouse IgM and IgG was added overnight at 4°C. Spots were developed with 3-amino-9-ethylcarbazole.

Metabolic flux analysis

Flow-sorted B cell populations (resting B cells, activated B cells and plasmablasts) from at least 3 Py-infected (day 10 p.i.) were plated at 250,000 cells per well in poly-lysine coated Seahorse XF96 cell culture microplate. Cells were allowed to adhere for 30 min to 1 h. OCR was measured in modified DMEM containing 2 mM L-glutamine (XF media) under basal conditions in a 96-well extracellular flux assay using a Xfe-96 (Seahorse Bioscience). In experiments comparing metabolic activity of B cell populations sorted from mice maintained on either regular water or water supplemented with L-glutamine, the culture medium was devoid of L-glutamine.

Metabolite measurements

Frozen spleens from naïve and Py-infected mice (∼40 mg) were lyophilized, extracted and analyzed as described previously⁵⁶. Briefly, gas chromatography/mass spectrometry were utilized for biochemical detection of metabolites by automated comparison of ion features in samples to a reference library of chemical standards entries, including retention time, molecular weight (m/z), preferred adducts, and in-source fragments as well as associated MS spectra.

Amino acid supplementation

Drinking water of Py-infected mice was supplemented (2.8 g/dL) with either L-glutamine, L-valine or L-alanine (Sigma Aldrich) starting at the indicated timepoints.

ELISA

Plates (Nunc Maxisorp) were coated either with 0.5 μg/mL MSP1₁₉ (MR4) or 18 μg/mL total parasite lysate and blocked with 2.5% BSA + 5% normal goat serum. After washing wells with ELISA wash buffer (PBS+ 0.05% Tween 20; 250 μL/ well, 3 min/wash), serially diluted serum samples from naïve and Py-infected mice were added and incubated for 18 h at 4 °C. Plates were washed and MSP1₁₉-specific or parasite specific antibodies were detected with HRP-conjugated goat anti-mouse IgG or IgG1 or IgG2b (in ELISA blocking buffer). After washing, plates were developed with SureBlue reserve TMB Kit (KPL) according to the manufacturer’s protocol and absorbance was at OD₄₅₀ using a Spectra Max 340 (Molecular Devices). End point titers were extrapolated from sigmoidal 4PL (where X is log concentration) standard curve for each sample. The threshold for end point titers is the mean plus 4–8× s.d. recored for naïve mouse sera.

For ex vivo CD138^hiIgD^neg B cell ELISA, 8 × 10⁴ CD19⁺CD138^hiIgD^neg plasmablasts were sort purified from day 10 p.i. mice and cultured in supplemented IMDM (10% FBS, 2 μM glutamine, 100 U/mL penicillin, 100 μg/mL streptomycin, 50 mM β-mercaptoethanol) in the presence of 5 ng/ml P. yoelii parasite lysates. Supernatants were recovered after 3 days of culture. CD138^hi B cell supernatants were diluted 1:2 and added to previously blocked total parasite lysate coated Nunc plates and processed as described above.

Cell staining and Flow cytometry

For cellular analyses of splenic cells, mouse spleens were forced through a 70 μm mesh to generate single-cell suspensions. The single-cell suspension of splenocytes were subjected to red blood cells lysis, were counted and resuspended at 10⁶ cells/100 μL. Fc receptors were blocked using Fc block/CD16/32 (clone 2.4G2) in FACS buffer (PBS+0.09% Sodium Azide +2% FCS) for 15 min at 4 °C followed by cell specific staining protocols as described below. For detecting GC-T_FH-like cells, cells were stained with purified rat α mouse CXCR5 (1:100; clone 2G8, BD Biosciences) in T_FH staining buffer (PBS+0.09% Sodium Azide +2% FCS+0.5%BSA+2% mouse serum) for 1 h at 4 °C. Cell were washed in FACS buffer, spun at 300 × g for 5 min at 4 °C and resuspended in Biotin SP-conjugated Affinipure Goat-anti-rat IgG (H+L) F(ab) (1:1000, Jackson Immunoresearch) in T_FH staining buffer and incubated for 30 min at 4 °C. Cell were washed in FACS buffer, spun at 300 × g for 5 min at 4 °C and resuspended in an antibody cocktail containing CD4-PercP Cy5.5 (1:300; clone GK1.5; BioLegend), CD44-AF700 (1:1000; clone IM7; BioLegend), CD11a-FITC (1:300; clone M17/4; BD Biosciences), PD-1-PE or PE-Cy7 (1:300; clone RMP1–14; BioLegend) and streptavidin-BV421 (1:500) and incubated 30 min at 4 °C. The cells were washed with FACS buffer as before and resuspended in FACS buffer before acquisition. For B cell staining, cell were stained with rat anti-mouse B220-PercP-Cy5.5 (1:300; clone RA3–6B2; BioLegend), rat anti-mouse CD19-AF700 or PE (1:300; clone 6D5; BioLegend), rat anti-mouse IgD-Pac Blue or BV510 (1:500; clone 11–26c.2a; BioLegend), rat anti-mouse CD138-APC or Pac Blue (1:250; clone 281–1; BioLegend) (for plasmablast staining); rat anti-mouse GL7-PE (1:300; BioLegend) and hamster anti mouse CD95-FiTC (1:300; clone Jo2; BD Biosciences) (for GC B cell staining); rat anti mouse CD23-PE Cy7 (1:300; clone B3B4; BioLegend) and rat anti-mouse CD21-APC (1:300; clone 7E9 BioLegend) (for marginal zone B cell staining). For human B cell staining, 200 μl of blood was stained with surface antibodies to CD19 (FITC, clone HIB19), CD27 (AF700, clone M-T271) CD38 (BV785, clone HIT2).

BrdU and FLICA Staining

BrdU (Sigma) was injected i.p. at 2 mg and supplemented in the drinking water at 0.8 mg/ml from days 6–10 p.i. FLICA reagent was prepared and added to cells according to manufacturer’s instructions (Thermofisher). For BrdU staining, cells were permeabilized, treated with 3 μg/mL DNAse (Invitrogen) and subjected to intracellular staining with either anti-BrdU-FITC (clone PRB-1) or mouse IgG1-FITC.

Statistical Analysis

Statistical analyses, end point titers, and overall parasite burden, represented as area under the curve for rodent studies were performed using GraphPad Prism 6 software (GraphPad). Specific tests of statistical significance are detailed in the figure legends.

Data Availability Statement

The data that support the findings of this study are available as Source Data files and from Gene Expression Omnibus GSE134548. All data are available from the corresponding author upon request.

Extended Data

Extended Data Fig. 1. Experimental malaria expands extrafollicular plasmablast populations.

a, Gating strategy for identifying plasmablasts (CD138^hiIgD^neg), activated (CD138^loIgD^neg) and resting B cells (CD138^loIgD^hi). b, kinetics of PB in blood. Data are means ± s.d, representative of n = 2 biologically independent experiments with similar results using n = 3 mice/time point. c, CD138^hiIgD^neg plasmablasts were sort-purified from Py-infected mice on day 10 p.i., cultured for 20 hours and parasite lysate-specific IgM and IgG secreting ASCs were detected. Representative wells of ELISPOT assay. d, Relative CD19 expression by CD138^hiIgD^neg plasmablasts on days 7, 10, and 14 post Py infection. Data are representative of n > 5 experiments with similar results. e, BrdU incorporation in CD138^hiIgD^neg plasmablasts was assessed on day 10 p.i. Histogram represents BrdU staining, solid gray histogram is isotype (mouse IgG1). Data are representative of n = 2 experiments with similar results using n = 8 mice. f, Forward scatter and side scatter of CD138^hiIgD^neg plasmablasts examined on day 10 p.i. Data are representative of n > 5 experiments with similar results. g, Blimp-1/eYFP reporter mice were infected with Py. CD138^hi Blimp-1/eYFP⁺ cells in bone marrow from naïve (left panel) or day 21 infected mice (right panel). Data are representative of n = 2 independent experiments with similar results using n = 4 mice/group. h,i, CD21 and CD23 expression by B cells in a naïve mouse (h) and day 10 Py-infected mouse (i) showing plasmablasts (green box) activated (blue box) and resting (red box) B cells. Data are representative of n > 5 experiments with similar results using n = 3 mice/group. j, Representative plots of the frequency and total numbers of GC B cells (GL7⁺CD95⁺) among plasmablasts, activated and resting B cell populations on day 10 p.i. Data are means ± s.e.m., representative of n = 3 experiments with similar results using n = 5 (Day 0 Total B cells) and n = 4 mice (each remaining group).

Extended Data Fig. 2. Developmental abrogation of blood stage Plasmodium infection-induced plasmablast responses.

a, Experimental design for adoptive transfers. b, Experimental design for Rosa26-ERT2/Cre × Prdm1^fl/fl (CD45.2) : μMT bone marrow chimeric system. Eight weeks after engraftment, mice were infected with 1 × 10⁶ Py and then treated with either corn oil or tamoxifen on days 4, 5, and 6 p.i. c, Gating strategy of T_FH cells. d, Kinetics of parasite burden in Py-infected wild-type mice treated with tamoxifen or corn oil on days 4, 5, and 6 p.i. Data are means ± s.e.m., pooled from n = 2 biologically independent experiments with n = 6 mice/group. e, Experimental design for the three-way mixed bone marrow chimera. f, Eight weeks after engraftment, mice were infected with Py, treated with either corn oil or tamoxifen on days 4, 5, and 6 p.i. and the relative proportions (pie diagram) of Prdm1^fl/fl (CD45.2) and wild-type (CD45.1) cells in the GC B cell compartment was analyzed. Data are means ± s.e.m., pooled from n = 2 biologically independent experiments with n = 4 mice/group. g, Evaluation of T_H1 responses in PBS and tamoxifen-treated mixed bone marrow chimeric mice (as shown in b). Data are means ± s.d. representative of n = 2 biologically independent experiments with similar results using n = 5 (corn oil) and n = 4 mice (tamoxifen). Data in f,g were analyzed using two-tailed Mann-Whitney. Symbols and symbols represent individual mice.

Extended Data Fig. 3. Deletion of blood stage Plasmodium infection-induced plasmablast responses.

a, Experimental design for generating CD138-DTR chimeras. Eight weeks after engraftment, mice were infected with 1 × 10⁶ Py and on days 5 and 7 p.i. treated with either DTx or PBS to delete plasmablasts. Data are means ± s.d., representative of n = 2 independent experiments with similar results using n = 4 mice/group. b-d, Py-infected wild-type mice were treated with either DTx or PBS on days 5 and 7 p.i. Kinetics of parasite burden (b), representative plots and summary data of GC B cells (c) and GC-Tfh cells (d) on 21 p.i. Data are means ± s.d., representative of n = 2 biologically independent experiments with similar results using n = 4 (PBS) and n = 3 mice (DTx). e-g, CD138-DTR chimeric mice were infected with 1 × 10⁶ Py, plasmablasts were deleted with DTx and mice were subsequently treated with either MR-1 (anti-CD40L) or hamster IgG on days 8–11 p.i. Representative plots and summary data of GC B (e) and GC-TFH (f) cells as measured on day 21 p.i. and kinetics of parasite burden (g). Data are means ± s.e.m., pooled from n = 2 biologically independent experiments with n = 6 mice/group. Symbols in c-f represent individual mice and data were analyzed using two-tailed Mann-Whitney.

Extended Data Fig. 4. Differentially expressed genes among splenic B cell populations.

a, Venn diagram showing differentially expressed genes assessed by RNA-seq among the three splenic B cell populations on day 10 p.i. Respective cell types were sort-purified from n = 4 Py-infected mice. Data were obtained from one RNA-Seq experiment. Two-tailed ANOVA was used for identifying differentially expressed genes. b, Heat map showing the relative expression of all annotated genes assessed using RNA-Seq. c, Heat map showing the relative expression of genes involved in the unfolded protein response pathway (UPR).

Extended Data Fig. 5. L-glutamine enhances GC responses during experimental malaria.

a, L-glut concentrations in the spleens of naive and Py-infected wild-type mice on day 5 p.i. Data are means ± s.d. representative of n = 2 biologically independent experiments with similar results using n = 3 mice/group analyzed by a two-tailed unpaired t test (DF = 4; t = 5.933). b,c, Kinetics of parasite burden in mice treated with either L-alanine (b, H₂O + L-ala), L-valine (c, H₂O + L-val) or water starting on day 0 p.i. Data are means ± s.d., representative of n = 2 independent experiments with similar results using n = 3 mice/group. d-f, Py-infected wild-type mice were treated with L-glutamine (H₂O + L-glut) or water starting day 0 p.i. and subsequently treated with MR-1 (anti-CD40L) or Hamster IgG antibody on days 8–11 p.i. Kinetics of parasite burden (d) and frequency of GC B cells (e) and GC-Tfh cells (f) on day 21 p.i. Data in d are means ± s.e.m, pooled from n = 2 independent experiments with n = 7 mice/group. Data in e,f are representative of n = 2 biologically independent experiments with similar results using n = 3 mice/group. g-m, Py-infected wild-type mice were treated with L-glutamine (H₂O + L-glut) or water starting day 0 p.i. Kinetics of GC B cells (g), class-switched GC B cells (h), plasmablasts (i), and GC-T_FH-like cells (j). Data in g-j are means ± s.d., representative of n = 2 biologically independent experiments with similar results using n = 6 mice/group analyzed by two-tailed Mann-Whitney. k, gMFI of BCL6 on GC-T_FH-like cells. Data are means ± s.d., representative of n = 2 biologically independent experiments with similar results using n = 3 mice/group analyzed by two tailed unpaired t test (DF = 4; t = 1.257). Number of T_H1 cells (l, Ly6C+CXCR3+IFNg+) and gMFI of CD80 and CD86 expression on splenic dendritic cells (m, MHCII+CD11c+) on day 10 p.i. Data in l,m are means ± s.e.m, pooled from n = 2 biologically independent experiments with n = 6 (H₂O) and n = 7 mice (H₂O + L-glut) analyzed by two-tailed Mann-Whitney. n,o, Kinetics of parasite burden (n) and area under curve as a measure of total parasite biomass (o) in Py-infected wild-type mice treated with L-glutamine (H₂O + L-glut) starting on day 6 p.i. Data in n are means ± s.d., representative of n = 2 biologically independent experiments with similar results using n = 4 mice/group. Data in n analyzed using two-way ANOVA with Sidak’s multiple comparison (DF = 5; F = 5.728). Data in o analyzed with two-tailed Mann Whitney. p,q, Kinetics of parasite burden (p) and area under curve (q) as a measure of total parasite biomass in Py-infected wild-type mice treated with L-glutamine (H₂O + L-glut) starting day on 10 p.i. Data in p,q are means ± s.d., representative of n = 2 independent experiments with similar results using n = 4 mice/group analyzed by two-tailed Mann Whitney. Symbols in a, l-q represent individual mice.

Extended Data Fig. 6. Experimental design for treating CD138-DTR: WT chimeras with L-glutamine.

Eight weeks after engraftment, mice were infected with Py and treated with L-glut or water starting on day 0 p.i. Mice were subsequently treated with either DTx or PBS on days 5 and 7 p.i. to delete plasmablasts.

Extended Data Fig. 7. Post-GC administration of L-glutamine does not appreciably enhance LLPC and MBC responses.

a, Gating strategy for long lived plasma cells (LLPCs) in the bone marrow of Py-infected mice. b, Numbers of LLPCs in the bone marrow on day 60 p.i. from Py-infected mice treated with either L-glutamine (H₂O + L-glut) or water (H₂O). Data are means ± s.e.m., pooled from n = 2 biologically independent experiments with n = 7 mice/group analyzed by two-tailed Mann Whitney. c,d, Py-infected wild-type mice were treated with either L-glutamine (H₂O + L-glut) or water (H₂O) at indicated time points p.i. and analyzed on day 30 p.i. Numbers of splenic memory B cells (c, CCR6+CD38+) and representative ELISPOT wells and summary data (d) demonstrating number of antibody-secreting LLPCs in the bone marrow. Data in c,d are means ± s.e.m, pooled from n = 2 biologically independent experiments with n = 5 (d, days 6–10) and n = 6 mice (remaining groups) analyzed by two-tailed Mann Whitney. Symbols represent individual mice.

Extended Data Fig. 8. Experimental design for the volunteer infection study.

Two thousand eight hundred viable P. falciparum infected RBCs were intravenously into malaria naïve healthy volunteers (n = 36 men, n = 4 women). On day 8 p.i., volunteers received anti-malarial drug treatment. On days 0, 8 (treatment day), 14/15 and 27/28/36 (end-of-study, EOS), blood samples were collected and plasmablasts were assessed by flow cytometry.