Preexisting IgG forms immune complexes and links local thermal reactogenicity with immunogenicity in influenza vaccination

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Hirsiger, Silke Scarascia, Mike Recher, Glenn Bantug, and 1 more This is a preprint; it has not been peer reviewed by a journal. https://doi.org/ 10.21203/rs.3.rs-8338543/v1 This work is licensed under a CC BY 4.0 License Status: Published Journal Publication published 02 May, 2026 Read the published version in npj Vaccines → Version 1 posted 14 You are reading this latest preprint version Abstract Pre-existing pathogen-specific antibodies shape vaccine outcomes, yet their impact on local reactogenicity and qualitative features of the immune response are not fully defined. In this prospective human cohort receiving seasonal influenza vaccination, high baseline hemagglutinin-specific IgG1 levels were associated with more pronounced local thermal responses at the vaccinated arm and greater vaccine-induced antibody levels. These IgG antibodies formed immune complexes with hemagglutinin, activated complement and enhanced Fc-receptor-dependent monocyte activation and phagocytosis in vitro , connecting pre-existing immunity to innate activation and local reactogenicity. Despite higher antibody levels and early plasmablast responses in subjects with strong thermal reactogenicity after vaccination, we observed lower avidity and hemagglutinin-inhibition capacity, suggesting extrafollicular responses. T cell responses were unaltered. These findings suggest an immune complex-mediated pathway through which pre-existing hemagglutinin-specific IgG amplify local thermal reactogenicity and modulate vaccine response quality, providing mechanistic insight into how prior immunity shapes human vaccine responsiveness. Biological sciences/Immunology Biological sciences/Microbiology Local reaction reactogenicity influenza pre-existing immunity vaccine response temperature monocytes FcR ADCP extrafollicular B cell response vaccine Figures Figure 1 Figure 2 Figure 3 Figure 4 Figure 5 Introduction Vaccination induces a pathogen-specific immune response to prevent subsequent infections. Protection is conferred by humoral B cell and T cell responses. Vaccine-specific B cells emerge from both follicular and extrafollicular pathways, leading to the development of either long-lived plasma cells and memory B cells, or short-lived antibody-secreting cells that provide rapid, yet temporary, immunological protection 1 . The determination of B cell response fate, whether follicular or extrafollicular, depends on the antigen type, T cell help, cytokine environment, and pre-existing memory from prior antigen exposure 1 , 2 . Generally, primary immune responses are characterized by extrafollicular plasmablasts that produce low-affinity antibodies, while some B cells migrate to germinal centers to undergo affinity maturation. Secondary responses involve follicular memory B cells that rapidly differentiate into plasma cells producing higher-affinity antibodies 3 , 4 . Humans are frequently exposed to respiratory viruses. For influenza, it is estimated that most individuals become infected at least once over six seasons 5 . Therefore, the seasonal influenza vaccine encounters a primed immune system with pre-existing antigen-specific antibodies and memory B cells 6 . Importantly, humoral responses to influenza vaccination can be diminished or enhanced by pre-existing immunity, depending on the antigen and the functional characteristics of the pre-existing humoral immunity 6 . While antibody-mediated protective immunity is primarily provided by neutralizing antibodies that block the virus from infecting cells 1 , it became evident that non-neutralizing antibodies exert various protective or modulatory functions in the vaccine response 7 . Through Fc-dependent pathways, such as antibody-dependent cellular phagocytosis (ADCP), cellular cytotoxicity (ADCC) or through complement activation (ADCA), these antibodies can label virions for uptake, shape antigen processing, and influence downstream adaptive responses 7 , 8 . There is increasing evidence that non-neutralizing anti-hemagglutinin (HA) antibodies contribute to influenza vaccine-induced protection 9 – 11 . In natural infections and immunizations with replication-competent viruses (e.g., vector or live attenuated vaccines), pre-existing immunity accelerates viral or vaccine virus clearance and can, in rare cases, facilitate antibody-dependent disease enhancement 12 , 13 . In contrast, vaccinations containing viral protein antigens rely on a high amount of antigen to surpass the antigenic threshold for effective immune priming 14 . FcR-dependent interactions of serum IgG with a protein antigen have been described, including the formation of immune complexes 15 , 16 . However, the extent to which distinct pre-existing anti-influenza antibody profiles can influence vaccine antigen uptake via Fc-mediated functions and, subsequently, the induction of the adaptive immune response to influenza vaccination, is poorly understood. Furthermore, how antibody-Fc-receptor-mediated pathways of innate immune activation contribute to reactogenicity has not been thoroughly examined. Local injection site reactions (ISR) are the most common adverse events following immunization. The local inflammation associated with ISR is mediated by innate immune activation; a crucial element in initiating the immune response to vaccines. Vaccine-mediated activation of pathogen- or damage-associated molecular patterns (PAMPs and DAMPs) leads to the release of pro-inflammatory cytokines, cell migration and antigen uptake via endocytosis or phagocytosis 17 . Local inflammation arises a few hours after vaccination and usually resolves within three days 17 . Pre-existing vaccine-specific immunity contributes to the vaccine reactogenicity, as evidenced by severe local reactions (‘hyperimmunization’) 18 or immune-complex-mediated reactions (Arthus reactions or type III hypersensitivity reactions) 19 . Few studies have investigated whether the reactogenicity of the influenza vaccine is associated with vaccine immunogenicity or efficacy. In heart failure patients, adverse events following influenza vaccination were associated with better cardiovascular outcomes 20 . A post-hoc analysis of an immunogenicity study observed stronger local reactions in subjects with low pre-existing immunity but a high antibody fold increase 21 . In studies of COVID-19 vaccines, fever, but not local reactogenicity, was associated with higher antibody levels 22 – 25 . Notably, none of these studies monitored local temperature reactions. Here, we studied the contributing immunological factors and consequences of local temperature reactions to seasonal influenza vaccination in a human model system with variable pre-existing immunity and reactogenicity. Results Influenza vaccination induced a local thermal reaction 24 hours post-vaccination Between November 2019 and January 2020, 38 healthy subjects who received the inactivated seasonal influenza vaccination were enrolled. The baseline characteristics of the study population are summarized in Table 1 . We measured temperatures at the temporal region (‘systemic temperature’) and the deltoid region (‘injection site’ and ’control site’) before and 24 hours following quadrivalent inactivated influenza vaccination (QIV) using a no-touch temporal thermometer (Fig. 1 A). The increase in skin surface temperature at the injection site was defined as the ‘local thermal reaction/reactogenicity’. Systemic temperature was unchanged 24h post-vaccination and comparable between the two temporal measurement sites (baseline median T temp(L) 36.85°C vs. T temp(R) 36.80°C, p = 0.90; 24h post-vaccination median T temp(L) 36.83°C vs. T temp(R) 36.88°C, p = 0.98) (Fig. 1 B). Vaccination induced a significant temperature increase at the vaccinated arm 24h post-vaccination (median T vacc 36.63°C vs. 35.90°C; p < 0.0001) but not at the control arm (median T ctrl 36.05°C vs. 35.95°C; p = 0.73) (Fig. 1 C). The median temperature increase at the vaccinated arm was higher in women (ΔT vacc24h−BL +0.63°C vs. +0.32°C in men, p = 0.04) (Fig. 1 D) and in those with a clinically observed local erythema (ΔT vacc24h−BL +1.55 vs. +0.35°C, p < 0.0001) (Fig. 1 E). The erythema diameter was correlated with the ΔT at the vaccine arm ( Supplementary Fig. 3, p < 0.0001, r = 0.68), and self-reported severe pain showed a significant correlation with the temperature increase (Fig. 1 F ) . The number of influenza vaccines received in the preceding five years had no influence (Fig. 1 G ). Table 1 Baseline Characteristics Total n = 38 Women, n (%) 27 (70.5%) Age, median (IQR) 31 (27-42.5) BMI, median (range) 21.9 (20.7–24.1) Vaccinated arm - left 34 (89.5%) - right 4 (10.5%) Medical history - Allergy* 15 (39.5%) - Autoimmunity** 3 (7.9%) - Current Smoker 1 (2.6%) ILI past 5 years - none 27 (70.5%) - previous year only 1 (2.6%) - > 1–5 years ago 10 (26.3%) Influenza vaccines (past 5 years) - 0 11 (28.9%) - 1 11 (28.9%) - 2 2 (5.3%) - 3 4 (10.5%) - 4 3 (7.9%) - 5 7 (18.4%) *RCA=allergic rhinoconjunctivitis, asthma, penicillin; **Basedow (n = 1), Psoriasis(n = 2); ILI= influenza like illness Pre-existing IgGs from subjects with subsequently augmented thermal reactogenicity potently activated monocytes Local injection-site reactions result from vaccine- or adjuvant-mediated innate immune activation. Immune complexes can trigger cytokine-independent monocyte activation via the Fc-receptor (FcR) or complement receptors. IgG1, the HA-specific IgG subclass that was significantly elevated in pre-immunization sera of ΔT hi subjects, potently activates FcR 27 . Accordingly, we examined whether the higher levels of anti-HA-IgG1 in ΔT hi subjects were associated with enhanced FcR-mediated monocyte activation or complement system activation. To test this, recombinant hemagglutinin was mixed with pre-vaccination sera to form HA-IgG immune complexes (HA-IgG-IC). Using a C1q-binding assay, we demonstrated that HA-IgG-IC from ΔT hi more robustly bound complement (Fig. 3 A), which was directly correlated with the amount of HA-specific IgG (H1: r = 0.73, p < 0.0001; H3: r = 0.72, p < 0.0001). Next, we used an in vitro complement activation assay that measures CD4d deposition by ELISA 28 . HA-IgG-IC from ΔT hi showed significantly stronger serum complement activation than HA-IgG-IC from ΔT lo (Fig. 3 B). The ADCP capacity of HA-IgG-IC formed with the pre-vaccination sera was assessed using fluorochrome-labeled hemagglutinin (HA fluo ) to monitor cellular uptake of HA fluo -IgG-IC. Using primary monocytes and pre-vaccination sera from ΔT hi and ΔT lo subjects, we observed an increased ADCP of HA fluo -IgG-IC by monocytes from ΔT hi subjects (Fig. 3 C). In contrast, there was no difference in HA uptake after FγR-independent monocyte activation by TLR4-stimulation with LPS, nor when the same experiments were conducted with mDCs (Fig. 3 C, Supplementary Fig. 7 ). We confirmed that IC uptake in this assay depended on a functional IgG/FcγR interaction using blocking antibodies against FcγRI (CD64), FcγRII (CD32), or FcγRIII (CD16), alone or in combination ( Supplementary Fig. 7 ). Overall, there was redundancy among the different FcγR, but blocking FcγRI most potently decreased IC phagocytosis. Complementary experiments using IgG-depleted sera or the serum of a subject with severe hypogammaglobulinemia further confirmed that HA uptake was mainly ADCP-mediated ( Supplementary Fig. 7 ). Next, we aimed to compare the ADCP function of the pre-vaccination sera in a controlled cellular system using the THP-1 cell line. Stimulation of the THP-1 monocyte cell line with pre-vaccination HA-IgG-IC from ΔT hi subjects induced significantly enhanced THP-1 activation (HLA-DR hi CD86 hi ), pro-inflammatory cytokine secretion (IL-1β and IL-6), and antibody-dependent phagocytosis (ADCP) compared to HA-IgG-IC from ΔT lo subjects (Fig. 3 D). The associations between the local thermal reaction and monocyte activation were comparable regardless of whether H3 or H1 was used as the hemagglutinin target (Fig. 3 D and Supplementary Fig. 8 ) and were confirmed using the absolute ΔT values in complementary correlation analyses ( Supplementary Fig. 8 ). ADCP and monocyte activation were closely connected to the levels of pre-existing HA-specific IgG1, the amount of HA-IgG-IC formed in vitro, and the clinically observed local thermal reactogenicity, which showed the strongest statistical correlation. ( Supplementary Figs. 9 and 10 ). In vivo , we observed differences in the frequency of peripheral blood monocytes amongst PBMC 24 h post-vaccination in ΔT hi vs. ΔT lo (median 10.0% vs. 17.7%, p = 0.009), with lower frequencies of classical (CD14 high CD16 neg ) monocytes (44.7% vs. 62.8%, p = 0.004) and an increased frequency of non-classical (CD14 low CD16 high ) monocytes (29.4% vs. 10.5%, p = 0.041) in ΔT hi ( Supplementary Fig. 11 ). These monocytes exhibited a higher median fluorescence intensity (MFI) of HLA-DR expression across all monocyte subsets (CD14 high CD16 negative , CD14 high CD16 low , and CD14 low CD16 high ), while CD86 was only elevated on CD14 high CD16 negative monocytes ( Supplementary Fig. 11 ). Inflammation-related heat likely results from hyperemia driven by local cytokine release, but it may also stem from cellular heat generation. We investigated this by measuring the temperature of the cell culture media in stimulated THP-1 cells using an immersion temperature probe. Monocytes of ΔT hi subjects produced significantly more heat in vitro (T 37.55°C vs. 37.76°C, p = 0.0159) when activated by autologous HA-IgG-IC, but not when non-specifically activated with LPS (Fig. 3 E,F). In addition, we employed a thermo-sensitive mitochondrial-targeted fluorescent dye, MitoThermo Yellow (MTY), to visualize mitochondrial temperature production at the cellular level in primary monocytes. In this assay, higher temperature production results in reduced MTY fluorescence intensity 29 . Differences in the mitochondrial temperature production were confirmed in the MTY assay comparing ΔT hi and ΔT lo HA-IgG-IC-mediated THP-1 cell activation (MTY MFI 1058 vs. 2562, p = 0.002) (Fig. 3 G). Immune cell heat generation was almost exclusively monocyte-derived ( Supplementary Fig. 11 ). Together, these results suggest that higher anti-HA-IgG1 pre-vaccination levels may drive FcR-dependent or complement activation mediated monocyte activation through IC, resulting in more pronounced local thermal reactogenicity, potentially affected by increased heat generation of immune complex-activated innate immune cells. Impact of temperature on B cell functions in vitro Thermal energy drives several immunological processes, including cell migration, cellular activation, cytokine secretion, and cell proliferation 30 – 33 . Although our data establish FcR-dependent monocyte heat generation in vitro , the extent to which such micro-scale thermal changes occur in vivo and reach the B cell niches remains to be defined. Nevertheless, these findings prompted us to examine how modest, transient temperature elevations might affect antigen-driven B cell activation. We performed experiments in temperature-controlled cultures to model the impact of in vivo inflammation-associated heat, hypothesizing that immune-complex activated innate immune cells may generate heat, as suggested by our in vitro data. To begin to explore this, we stimulated pre-vaccination PBMC with the QIV at 37°C and 39°C for five days and monitored in vitro B cell proliferation and differentiation into CD27 high CD38 high plasmablasts (PB). The detailed B cell gating strategy is shown in Supplementary Fig. 1 . QIV-stimulated B cells cultured at 39°C exhibited four-fold higher PB frequencies (36.5% vs. 9.6%, p = 0.0039; Fig. 4 A) and more than two-fold increased proliferation (50.2% vs. 20.5%, p = 0.0039; Fig. 4 B) compared to cells cultured at 37°C. Notably, we did not observe any effect of culture temperature when using non-BCR-mediated B cell stimulation with CD40L/IL-21 (Fig. 4 A,B). Activating B cells with QIV at elevated temperatures enhanced polyclonal IgG production (Fig. 4 C), resulted in a mild increase in IgM ( Supplementary Fig. 12 ), and was associated with a significant increase in influenza strain-specific IgG (Fig. 4 D). However, HA-specific antibodies produced at 39°C had a lower avidity index in urea challenge assays than those produced at 37°C (0.81 vs 0.34, p = 0.0039, Fig. 4 E). These findings suggest that an elevated temperature in the microenvironment of B cells promotes antigen-induced B cell activation, proliferation, and antibody secretion. A strong thermal reactogenicity associated with a high magnitude but low-avidity and poorly hemagglutinin inhibiting IgG response in vivo The thermal reaction at the vaccination site transiently exposes immune cells to elevated temperatures. Given the in vitro evidence that heat modulates B cell activity, we next examined whether vaccine-induced immune responses differed between individuals with high (ΔT hi ) and low (ΔT lo ) thermal reactivity. We assessed the frequencies of plasmablasts and T follicular helper (Tfh)-like T cells in the peripheral blood on day 7, along with T cell responses, antibody levels, HAI titers, and antibody avidity on day 28. An unsupervised hierarchical clustering analysis revealed that thermal reactogenicity, pre-vaccination HA-specific IgG1, and immune complex formation were strongly interconnected and associated with features of an extrafollicular B cell response (Fig. 5 A). Subsequently, we performed direct group comparisons between the ΔT hi and ΔT lo groups. Plasmablast egress from lymph nodes and the expansion of circulating Tfh-like T cells are hallmarks of the early influenza vaccine response in humans 34 , 35 . At baseline and on day 7, Tfh-like cell frequencies were comparable across groups (Fig. 5 B). In contrast, ΔT hi subjects exhibited significantly higher frequencies of circulating plasmablasts at 7 days post-vaccination (Fig. 5 C) and a more significant fold change compared to baseline (median: ΔT lo 9.250 vs. ΔT hi 15.96 fold change, p = 0.013). T cell intrinsic HA-specific IFNγ production at day 28 post-vaccination was non-significantly elevated in ΔT hi subjects (H1 + H3 408 vs 544 SFC/M, p = 0.3; QIV 510 vs. 629 SFC/M, p = 0.2) (Fig. 5 D). On average, the total hemagglutinin-specific IgG, specifically IgG1, against the vaccine strains at 28 days post-vaccination was 4-fold higher in subjects that exhibited strong thermal reactions (range 3.67–4.22-fold higher in ΔT hi subjects) and correlated with the absolute temperature increase at the vaccination site (Fig. 5 E, Supplementary Fig. 13) . In contrast, post-vaccination sera from subjects with mild thermal reactogenicity demonstrated greater hemagglutinin inhibition titers (as a surrogate for virus neutralization capacity) against the H1 and H3 vaccine strains (Fig. 5 F). Divergence in antigen-binding and neutralization capacity may be due to differentially targeted epitopes or to differences in antibody avidity. We found that vaccination-induced influenza-specific IgGs in ΔT hi subjects were of lower avidity than in those with mild thermal reactogenicity, as assessed by biolayer interferometry and urea challenge (Fig. 5 G, Supplementary Fig. 13 ). The QIV induced HA-specific IgG of all subclasses, but subclass distributions varied by HA specificity and thermal response profile, with IgG1 dominance in ΔT hi sera ( Supplementary Fig. 13 ). We then tested the d28 post-immunization serum for HA-IgG-IC-mediated THP-1 activation. HA-IgG-IC formed with post-vaccination (day 28) sera robustly activated THP-1 and enhanced ADCP, particularly when derived from ΔT hi individuals (Fig. 5 H). All key findings were confirmed in complementary analyses using ΔT and the vaccine response readouts as continuous variables ( Supplementary Fig. 14 ). These data collectively link increased thermal reactogenicity to elevated pre-existing, non-neutralizing (i.e., low HAI titers) anti-HA antibodies that promote the formation of IgG1-enriched immune complexes. This Fcγ receptor- and/or complement-mediated activation was associated with higher antibody magnitude post-vaccination. These antibodies had lower avidity and exerted lower hemagglutinin inhibition, suggesting that local heat and immunecomplex-driven inflammation shape the qualitative outcome of the vaccine response. Discussion Local reactogenicity is the most common adverse event following immunization, yet its immunological basis and consequences remain incompletely defined. In healthy adults receiving the seasonal influenza vaccine, we quantified the local temperature increase at the injection site and leveraged its broad inter-individual variability to dissect potential mechanisms underlying this response and its impact on adaptive immunity. Specifically, influenza vaccination triggered a measurable thermal reaction at 24 hours, enabling classification into high (ΔT hi ) and low (ΔT lo ) responders. We found that immune complexes formed between HA-specific IgG and recombinant hemagglutinin bound and activated complement in vitro . Similarly, HA-IgG-IC activated innate cells by engaging FcγR, thereby prompting monocyte activation, upregulating activation markers (HLA-DR and CD86), secreting inflammatory cytokines, and enhancing ADCP. The ΔThi subjects showed significantly higher levels of HA-specific IgG1 before vaccination. Additionally, the immune complexes with their serum exhibited significantly stronger FcγR-dependent immune activation and phagocytosis in monocytes. This underscores the role of pre-existing non-neutralizing IgG in promoting local inflammatory responses. These results diverge from a recent report that associated low baseline immunity with increased reactogenicity, although the lack of temperature measurements in that study limits direct comparison 21 . Moreover, we cannot exclude that other pathogen-specific IgG subclasses are more relevant than IgG1 in other vaccines or other clinical contexts. Conceptually, the pre-existing IgG against HA, forming HA-IgG-IC following immunization with HA and causing immune activation, represents a type III hypersensitivity (Arthus-like) reaction 19 . Unlike classical type III hypersensitivity, observed after exposure to an intravenous antigen that allows ICs to distribute to joints or other organs, the vaccine reaction is limited locally. Notably, the local thermal reaction, the baseline HA-specific IgG1, the HA-IgG-IC and FcR-mediated monocyte activation and ADCP were closely interlinked, and the amount of HA-IgG-IC correlated with the same baseline and outcome parameters as the ΔT ( Figure S9 and Fig. 5 A). Therefore, our study design prevents us from isolating the effects of immune complex-mediated complement activation and FcR-mediated monocyte activation on local heat production and reactogenicity. However, our data suggest that the overall innate activation is reflected clinically in the local thermal response, which serves as an easy, measurable, quantitative surrogate. The second key finding was that the local thermal reactivity was associated with downstream adaptive responses. Exploratory experiments using elevated culture temperatures in vitro showed enhanced B cell proliferation, plasmablast differentiation, and antibody secretion, in line with emerging evidence that heat affects immune cell dynamics and trafficking 30 . These in vitro experiments, however, were only an approximation of the in vivo situation and did not investigate other plausible mechanisms by which temperature could affect adaptive immunity, such as accelerated antigen uptake and processing. In vivo , ΔT hi individuals mounted higher HA-specific total IgG and IgG1 responses by day 28, however, these antibodies exhibited reduced avidity in biolayer interferometry and urea-challenge assays and exhibited weaker hemagglutinin inhibition capacity (as a surrogate for neutralization). Collectively, this data suggests that heightened local inflammation may increase antibody quantity at the expense of avidity. Previous studies have reported higher local reactogenicity and immunogenicity in women; however, most examined mRNA or adjuvanted vaccines and did not quantify local thermal responses, limiting direct comparison 36 . Fever after influenza vaccination has been associated with higher hemagglutination inhibition titers 37 , however, no participants in our study developed fever. Gromer at al. reported that local reactions were associated with lower pre-existing IgG levels, although local thermal responses were not assessed 21 . The inactivated influenza vaccine has an excellent safety profile, but local reactogenicity is common (30–50% of vaccinated subjects) 38 . Traditional studies investigating associations between reactogenicity and immunogenicity have relied on easily accessible measures such as pain, swelling, or fever. However, these are subjective, difficult to quantify, or may depend on the vaccine administration technique 39 . Temperature measurement provides an attractive, objective, and quantifiable alternative. Prior work using infrared imaging similarly reported heterogeneous thermal responses, yet without evaluating their immunological consequences 40 . They reported a mean temperature increase of + 0.70°C at 24h post-vaccination, with 40% experiencing a thermal reaction of at least + 1°C. Our in vitro data further suggest that immune cells themselves may contribute to local heat production, potentially via mitochondrial uncoupling. Mitochondria physiologically maintain temperatures that exceed core body temperature, which may reach 50°C in activated mitochondria 41 . The relevance of these mechanisms to vaccine reactogenicity remains to be further defined. The observation that pre-existing immunity shapes the adaptive vaccine response is not novel. The concept of antibody feedback summarizes the interference of pre-existing antigen-specific antibodies with the subsequent evolution of adaptive immunity upon revaccination or reinfection 6 . Thereby, immune complexes can enhance antigen uptake and presentation, potentially resulting in a more efficient antigen presentation and a more robust adaptive immune response 42 . However, antigen uptake in macrophages may limit antigen availability for B cell activation and sustained germinal center engagement. Similarly, pre-existing antibodies may mask epitopes, potentially promoting high-affinity B cell responses 43 , select for B cell responses against subdominant or less conserved epitopes (32), or prevent antigen uptake or B cell stimulation through interference 13 , 44 , 45 . However, our data do not support this hypothesis, as increased IC uptake was associated with an extrafollicular response phenotype with low-avidity antibodies on day 28. The HA-IgG-IC associated enhanced FcR-mediated innate activation, including monocyte activation, shapes the inflammatory milieu at the vaccination site. Strong innate inflammation associated with a features of a extrafollicular B cell response in our clinical cohort. Specifically, we observed a pronounced early plasmablast response at day 7 post-immunization and lower-avidity HA-specific IgG at day 28, in relation to strong thermal reactions. In this context, elevated local temperature may act as a modulatory factor rather than a primary driver, potentially influencing cellular metabolism, activation kinetics, or antigen processing during early immune response events. As a complementary explanation, accelerated extrafollicular responses may be fueled by preferential activation of memory B cells primed from prior influenza exposures, potentially further limiting the amount of antigen available for prolonged germinal center reactions and de novo affinity maturation. Future research should evaluate the baseline level of HA-specific memory B cells to explore their role in competing for and scavenging antigens. Including BCR sequencing data will help determine whether germinal center reactions are altered in individuals with strong local thermal reactions. Finally, vaccine antigen-IgG immunocomplexes increase the size and valency of the vaccine antigen. High-valency antigens induce a low-affinity, extrafollicular response, whereas smaller, low-valency antigens activate the high-affinity B cells preferentially 46 . Collectively, these mechanisms may explain the observed phenotype of extrafollicular B cell responses in those with a strong local temperature reaction and strong IC activation. Studies with IC-based vaccine strategies and Fc-engineered HA-Fc constructs have demonstrated that antibody glycosylation and Fc configuration can profoundly influence B cell selection, raising the possibility that qualitative features of pre-existing antibodies, not only their abundance, modulate vaccine outcomes. HA-IgG-IC have been explored as potential vaccine constructs in preclinical models and in humans 47 – 49 . In vivo , human influenza vaccine efficacy correlated with the amount of sialylated Fc on anti-HA-IgG produced during the early plasmablast response. The authors demonstrated that this improved humoral vaccine response occurs through co-engagement of the sialylated Fc region with CD23, which triggers the inhibitory FcγRIIB. This process raises the antigenic threshold and favors the selection of high-affinity B cells cells 50 . In preclinical studies, ICs consisting of the influenza vaccine and sialylated Fc anti-HA-IgG were used to immunize mice. IC vaccination elicited higher-avidity antibody responses than HA alone, with qualitatively enhanced breadth and potency against influenza viruses 51 . A modified approach to harnessing IC in influenza vaccination is fusing HA to an Fc fragment. Immunization with these fusion proteins induced broad immune responses and high cross-clade protection in mice 52 . Combined, this suggests that not only the amount of pre-existing IgG, but also the glycosylation of the Fc part, which critically informs the effector function of the IgGs, are important to consider. Our study's strengths include the integration of in vivo and in vitro systems and the detailed temporal profiling, which allows us to unravel associations between immune features and the reactogenicity phenotype. We investigated immune complex-mediated immune activation in mechanistic detail and demonstrate that immune cells may produce heat in vitro in a multi-modal approach. Limitations include the sample size, absence of a validation cohort, and female predominance in the ΔT hi subjects. We, therefore, cannot exclude that sex, hormonal differences, or relatively higher vaccine doses (per body mass compared to men) contributed to the observed phenotype. Notably, many immune genes are located on the X chromosome, including the innate sensor TLR7 53 and the literature consistently reports higher local reactogenicity and immunogenicity to the inactivated influenza vaccine in females (reviewed in 54 ). In contrast, systemic reactions occur with similar frequencies. Sex-related differences in hormones, skin thickness, blood flow, and the nervous system's structure may promote the development of injection-site inflammation in females 54 . Experimental limitations include that we only assessed immune complex formation and activation indirectly in vitro , as we did not perform muscle biopsies. Similarly, since direct assessment of neutrophil recruitment requires tissue sampling or whole-blood analysis, we focused on monocytes as an innate cell subset. Histopathological studies on local vaccine reactogenicity have been done mostly for specific vaccines. In humans, a combined PET/CT and needle biopsy study for transcriptomics investigated gene signatures following intramuscular immunization with an adjuvanted, but not the standard, influenza vaccine 55 . Mouse studies compared histopathologic findings one month post-immunization with various vaccines, including the influenza vaccine. The timing of sampling and the absence of pre-existing immunity in this animal study preclude conclusions regarding immune complex formation 56 . Whether it is appropriate to perform muscle biopsies in human volunteers following a seasonal influenza vaccine for research purposes is debatable. Animal models with pre-existing pathogen-specific immunity could be employed to study local immune complex formation and complement activation in the future. Finally, we cannot exclude that affinity maturation in subjects with strong local reactogenicity follows a different trajectory that was missed due to the single later timepoint at 28 days post immunization. Studies in humans have shown that following repeated immunization with the flu vaccine, affinity maturation is limited and often completed within four weeks 57 , 58 but can extend over months 59 . In conclusion, our study provides novel insights into the relationship between vaccine reactogenicity and pre-existing humoral immunity in standard, non-adjuvanted influenza protein vaccination. The findings underscore the importance of considering both the magnitude and quality of the immune response when evaluating the consequences of vaccine-induced reactogenicity. Further research is necessary to determine whether adjusting the thermal response at the injection site or via metabolic interventions can improve vaccine efficacy by balancing reactogenicity and immunogenicity. Conducting a clinical study to assess if non-steroidal anti-inflammatory drugs (NSAIDs) influence local thermal reactogenicity and subsequent immune responses would be relatively simple. Interestingly, in pediatric studies, NSAIDs did not significantly affect antibody responses to various vaccines vaccines 60 , 61 , although none of these studies tested antibody avidity or HAI titers as functional outcomes. Understanding how local inflammation and IC-driven pathways modulate vaccine immunogenicity may inform strategies to optimize antigen design, Fc engineering, and formulation to enhance protective immunity while limiting unwanted reactogenicity. Methods Study participants The local ethics committee (Ethics Commission of North-Western and Central Switzerland, EKNZ #2017 − 01726) approved the study (ARIVA-Study; NCT04059991, registration date on ClinicalTrials.gov: 2017-11-01) that was conducted in accordance with the Declaration of Helsinki. All subjects were healthy, provided written informed consent, and received no other vaccinations during the study. None of the study participants reported use of non-steroidal anti-inflammatory drugs (NSAIDs) during the 24 hours after the vaccination, or was taking corticosteroids, biologics, or other immunomodulatory medications. The majority of participants were healthcare workers or laboratory personnel. All subjects were vaccinated between November and December 2019 with the same inactivated, non-adjuvanted, quadrivalent influenza split vaccine (Vaxigrip Tetra, Sanofi 2019/20), containing 15 µg hemagglutinin per strain (A/Brisbane/02/2018; A/Kansas/14/2017; B/Colorado/06/2017; and B/Phuket/3073/2013) in a total volume of 0.5 mL. We gathered data through a questionnaire on self-reported influenza-like illness over the last five years, the total number of influenza vaccines received during this period, personal histories of allergic diseases and autoimmunity, and demographic details including sex, BMI, and age. Assessment of reactogenicity and local thermal reactions. We utilized a contact-free temporal thermometer (Withings, Europe) for all temperature assessments. According to the company, this thermometer employs 16 infrared sensors to take over 4,000 measurements within seconds (HotSpot Sensor Technology). It operates within a range of 35°C to 43.2°C (95°F to 109.8°F), featuring a resolution of 0.1°C (0.2°F and a clinical accuracy of ± 0.2°C (± 0.4°F) for measurements in the temporal area. We measured the temperature at the vaccine injection site (deltoid region) immediately before and 24 hours after vaccination, as well as at the same location on the opposite arm and both temporal regions (i.e., systemic temperature) for comparison. Measurements were conducted in duplicate, and average values were calculated to determine the temperature difference before and after vaccination at the injection site [ΔT (24h-0h)], between the vaccinated and control arm [ΔT(vaccine)-(control)], or systemically. The ‘local thermal response’ was defined as the ΔT at the vaccination arm. In addition, study participants subjectively rated their pain 24 hours post-vaccination as: none, mild, or strong. We examined the vaccination site for erythema (redness) and, if present, measured the largest diameter in centimeters (cm). Sampling and peripheral blood mononuclear cell (PBMC) isolation We collected serum and ethylenediaminetetraacetic acid (EDTA) blood samples before, after 24 hours, and on days 7 and 28 post-vaccination for immunological analyses. To isolate the PBMC fraction, the EDTA blood was diluted in PBS and layered over 16.5 ml Lymphoprep medium (density 1.077 g/ml) in centrifuge Leucosep tubes (Grainer Bio-One, Austria). PBMCs were isolated by standard Ficoll-Paque density-gradient centrifugation at 700×g for 15 minutes with a low acceleration and no breaks 62 . The enriched PBMC layer was collected and washed twice in PBS, and cells were used immediately or cryopreserved in FBS containing 10% DMSO until further use. Elispot to measure influenza-specific T cell responses Standard IFN-γ Elispot was performed using 150,000 PBMC/well. We stimulated the cells with 1µg/ml recombinant hemagglutinin (A/Brisbane/02/2018 (H1N1) and A/Kansas/14/2017 (H3N2)) (both from (eENZYME LLC, Gaithersburg, MD, USA) or with the commercial influenza vaccine (QIV; Vaxigrip Tetra, Sanofi 2019/20) in a 1:200 dilution on a IFNγ-coated PVDF (polyvinylidene fluoride) plate (Mabtech, Nacka Strand, Sweden) at 37°C, 5% CO 2 for 18 hours. 0.5 µg/mL SEB (staphylococcal enterotoxin B) for polyclonal T cell activation or media alone served as controls. Elispot data were expressed as spot-forming cells per million PBMC (SFU/M). Measurement of the influenza-specific antibodies by multiplexed Luminex assay Using a custom-made Luminex assay, we quantified antibodies specific to the H1 and H3 vaccine strain. Different Luminex MaxPlex®beads were coated with recombinant hemagglutinin (HA) from the vaccine strains A/Brisbane/02/2018 (H1N1) and A/Kansas/14/2017 (H3N2) according to the manufacturer’s instructions. Briefly, 1.25µg of HA protein was coupled onto 1.25 million beads in 500µl of 50 mM MES buffer (pH 5.0) for 2h at RT with constant rotation. The bead coupling to different HA was verified using an anti-His antibody (1 µg/mL, A00174, GenScript) and a PE-labeled anti-rabbit IgG secondary antibody (1 µg/mL, 406421, BioLegend) that detects the his-tag on the HA. To measure HA-specific serum IgG, we incubated 1000 beads with sera diluted 1:100 and following the manufacturer’s instructions 63 . We used 1 µg/mL of the respective mouse anti-human detection antibodies to quantify Influenza-specific IgM (SA-DA4), IgG (JDC-10), IgG1-4 subclasses (HP6001, HP6002, HP6050, HP6025) and IgA (2053-01; all from SouthernBiotech, Birmingham, AL, USA). Bovine serum albumin (BSA)-coated beads were the negative control. Data was acquired as median fluorescence intensity (MFI) on a Luminex 200 reader. To compare subclass-specific responses between groups, we calculated relative responses per immunoglobulin class and antigen, i.e. median MFI ΔT hi divided by MFI ΔT lo . Hemagglutination inhibition assay We measured influenza strain-specific hemagglutination inhibition (HAI) titers against A/Brisbane/02/2018 (H1N1) and A/Kansas/14/2017 (H3N2) (NIBSC, Hertfordshire, UK) 64 . The influenza virus concentration was adjusted to four hemagglutination units (HAU) in a standard hemagglutination assay. Pre- and post-vaccination sera were treated with a receptor-destroying enzyme (Denka Seiken Co., Ltd, Tokyo, Japan) for 18 hours at 37°C, followed by heat-inactivation at 56°C for one hour. Samples were diluted two-fold serially in PBS in duplicates and mixed 1:1 with the virus. After one hour at 37°C, formaldehyde-fixed guinea pig red blood cells (1.5%) were added and incubated for one hour at 4°C 64 . The HAI titer was defined as the highest serum dilution that inhibited hemagglutination. Hemagglutinin-IgG immune complex formation, C1q binding assay and in vitro complement activation Hemagglutinin-IgG immune complexes (HA-IgG-IC) were generated by mixing the recombinant HA at 0.5µg/mL HA (HA used as described above) with participants’ sera at a 1:10 dilution. Complement binding capacity of the HA-IgG-IC was assessed using the QUANTA Lite C1q CIC ELISA (Inova Diagnostics/Werfen, Barcelona, Spain) following the manufacturer’s instructions. Briefly, HA-IgG-IC were incubated in C1q-coated microplate wells, and C1q binding of the IC was detected using a horseradish peroxidase–conjugated goat anti-human IgG antibody and quantified by measuring absorbance at 450nm. Immune complex concentrations were extrapolated from the calibration curve and expressed as heat-aggregated human IgG equivalents per mL (µg Eq/mL). To assess in vitro complement activation, we coated plates with 5 µg/mL C1q protein (Complement Technology Inc., Tyler, TX, USA) in 0.2 M carbonate buffer (pH 9.6) overnight at 4°C., blocked with PBS + 1% BSA. Serum samples were diluted 1:50 in either HBS (HEPES-buffered saline) or PBS supplemented with 10 mM EDTA and incubated on the plates for 1 h at 37°C with shaking at 300 rpm. Complement activation was assessed by detecting C4d deposition using rabbit anti-human C4d (Abcam, Cambridge, UK, 1:400) followed by HRP-conjugated donkey anti-rabbit IgG (BioLegend, San Diego, CA, USA, 1:4000) and TMB substrate (Invitrogen, Waltham, MA, USA), and absorbance was measured at 450 nm 28 . Antibody avidity determination using Biolayer Interferometry (BLI) and urea challenge To assess anti-HA-antibody avidity by biolayer interferometry, 10 µg/mL His-tagged hemagglutinin (A/Brisbane/02/2018 (H1N1) and A/Kansas/14/2017 (H3N2)) was loaded onto Ni-NTA biosensors (Sartorius, Göttingen, Germany) in running buffer (PBS, 0.02% Tween-20, 0.1% BSA) for 300 s. Sensors were dipped in running buffer for 60 s, then into serum-containing buffer for association (300 s), followed by dissociation in buffer for 600 s. Regeneration involved three cycles of 20 mM glycine in PBS, alternating with running buffer, followed by reactivation in 20 mM NiCl₂ for 120 s. All steps were performed at 1000 rpm. KD values were calculated using Octet® CFR software (ForteBio, Fremont, CA, USA). In select experiments, IgG avidity was assessed in addition (or solely) by urea challenge, comparing Luminex MFI values of HA-specific IgG after 30 min incubation with either PBS or 6 M urea (room temperature, 800 rpm). The avidity index (AI) was defined as [MFI with incubation in urea solution] / [MFI with incubation in PBS]. Monocyte phenotyping, in vitro maturation and antibody-dependent cellular phagocytosis assay Primary monocytes were isolated from PBMC taken at the pre-vaccination timepoint from subjects with low and high local temperature reactions. Monocyte subsets were sorted on a FACSAria® III (BD Biosciences) using CD3 (Alexa Fluor 700, OKT3), CD19 (Alexa Fluor 488, HIB19), CD14 (FITC, 63D3), CD16 (BUV 496, 3G8), and a viability dye (eFluorTM 780, Invitrogen™). Sorted monocytes or the monocyte cell line THP-1 (ATCC® TIB-202™) were differentiated into monocyte-derived dendritic (mDC) cells for five days in the presence of 1000 U/ml GM-CSF and IL-4 each, replenished at days 2 and 4. For mDC maturation, 200 pg/ml LPS was added for 24 hours. Ex vivo monocytes and mDCs were incubated with fluorochrome-coupled hemagglutinin in the presence or absence of sera (1:10) from subjects with low- or high-temperature reactions, for four hours. Fluorochrome-coupling of the H3N2 A/Kansas/14/2017 hemagglutinin (10 µg/reaction) was performed using the Lightning-Link® Allophycocyanin (APC) conjugation kit (Expedeon, San Diego, CA, USA) according to the manufacturer’s instructions. Briefly, 10ug hemagglutinin was mixed with the Modifier reagent at a ratio of 1:10. The antibody-Modifier mixture was added directly to a vial containing lyophilized fluorochrome conjugation mix (APC) and resuspended by gentle pipetting. The reaction was incubated for 3 h at room temperature in the dark. Following incubation, Quencher reagent was added at a 1:10 ratio, gently mixed and incubated for 30 min at room temperature. The resulting conjugated antibody was ready for use without further purification. Activation and HA uptake were assessed by flow cytometry. Antibodies used to characterize the monocyte activation profile are listed in Supplementary Table 1. A viability dye (eFluorTM 780, Invitrogen™) was included in all experiments. In vitro cytokine production was quantified in the culture supernatants of monocytes activated as indicated in the respective experiments. We used ELISA kits for IL-1 and IL-6 (Peprotech, Cranbury, NJ, USA) according to the manufacturer’s instructions. For the Fc-receptor blocking experiments, we used antibodies against FcγR1 (CD64, 10.1) [10 µg/ml]), FcγR2 (CD32, FUN-2) [10 µg/ml]), and FcγR3 (CD16, 3GB) [10 µg/ml]) (all from BioLegend). THP-1 monocytes were preincubated with blocking antibodies for one hour before adding fluorochrome-labeled hemagglutinin and serum. The effect of blocking was calculated as percent inhibition ((H3 uptake without blocking / H3 uptake with the Fc block)*100). After four hours of incubation, cells were stained using antibodies listed in Supplementary Table 1 and acquired on a BD LSRFortessa. Analysis was performed using FlowJo v.20.6.2. In vitro temperature measurements of cellular heat production THP-1, PBMCs, or sorted cell subsets were resuspended in complete RPMI medium and transferred into a DeepWell 96 U well plate. After an acclimatization period of 1 hour at 37°C, the cells were stimulated with HA-IgG-IC, LPS [1ng/ml, for monocyte activation], CpG [1 µg/ml, for B cell activation], anti-CD3/CD28 antibodies [2 µg/ml, for T cell activation], PMA [0.1 µg/ml, for NK cell activation] or maintained in the medium as a control. The temperature of the culture medium was recorded every minute during the acclimatization period and a three-hour stimulation using a data logger thermometer (SEFRAM9814 Datenlogger-Thermometer) with a liquid-compatible immersion probe (TC type K. Testo). The average temperature for the entire three-hour period was summarized in bar graphs. Mitochondrial temperature production assay using MitoThermo Yellow (MTY) THP-1 or human primary monocytes were stimulated with the quadrivalent influenza vaccine [1:200] or LPS [1ng/ml] for six hours at 37°C, 5% CO 2 . Cells were then stained with 100nM MTY, 100nM MitoTracker Green (Invitrogen, Waltham, MA, USA), or both for 20 minutes at 37°C and 5% CO 2 . After washing, the cells were fixed and permeabilized with the BD fixation and permeabilization solution, and counterstained with DAPI (Biolegend, San Diego, CA, USA). Cells were mounted with Vectashield fluorescence mounting medium (Vector Laboratories, Burlingame, CA, USA) and analyzed using the Nikon A1 confocal microscope with a 100x oil-immersion objective (Nikon Plan Apo 100x 1.45NA oil). Stacked images were acquired at 0.1 mm intervals throughout the cell body. The fluorescence intensity of MTY overlapping with MitoTracker staining was quantified using ImageJ (Fiji, v.2.9.0). Data are expressed as MFI. Temperature effects on B cell function in vitro To study the direct effects of higher temperature on immune cells, specifically B cells, we performed experiments at different cell culture temperatures. To this end, we set the incubator temperature set-point to 37.5°C or 39°C. The 39°C was chosen to approximate the elevated tissue temperature at the vaccination site. The estimate was based on the observed increase in skin surface temperature. The readouts focused on B-cell functions. PBMCs from the pre-vaccination time point were stimulated with the influenza vaccine (Vaxigrip®) [1/200] or a combination of CD40L [100 ng/ml] and IL-21 [100 ng/ml] at 37°C or 39°C. To assess proliferation, PBMCs were stained with the CellTrace™ Violet Cell Proliferation Kit (Thermo Fisher Scientific, Waltham, Massachusetts, USA) according to the manufacturer’s instructions before stimulation. On day five, proliferation was quantified as %CTV low B cells among total B cells and plasmablast generation was assessed using antibodies listed in Supplementary Table 1 and a viability dye (eFluor™ 780, Invitrogen™). All flow cytometric experiments were acquired on an LSRFortessa (BD Biosciences, San Jose, CA) and analyzed using FlowJo (v.10.6.2). Total antibody production in the cultures was assessed after 7 days using an IgG and IgM ELISA (Invitrogen, Waltham, Massachusetts, USA). The influenza-specific IgG levels were measured using the multiplexed Luminex assay as described. Direct ex vivo immune cell phenotyping Peripheral blood mononuclear cells (PBMC) were stained immediately following isolation (as described above) for immuophenotyping. The antibodies used for in vivo T cell, B cell, and Monocyte phenotyping are listed in Supplementary Table 2 . A viability dye (eFluor™ 780, Invitrogen™) was included in all panels. All samples were acquired on a BD LSRFortessa (BD Biosciences, San Jose, CA) and analyzed using FlowJo v.10.9.0. Gating strategies are indicated in the Supplementary Figs. 1 and 2 . Data analysis and statistics Group comparisons were performed using non-parametric, two-tailed t-tests (Mann-Whitney). We considered p-values < 0.05 statistically significant and reported the detailed p-values in the results and figure legends. Correlations of continuous variables were assessed using the non-parametric Spearman’s rank correlation. Comparisons of more than two groups were done using one-way ANOVA and Dunn’s test. Data was visualized using GraphPad Prism (Version 10.4.2). Declarations Competing Interest Statement The Authors declare no competing financial or non-financial interest in relation to the study. C.T.B. is chair of the Swiss National Immunization Technical Advisory Group (NITAG). Author Contribution J.R.H. performed experiments/generated data, analyzed and visualized the data, and drafted the manuscript. S.S. recruited and sampled subjects and coordinated the study. G.B. and M.R. provided support in designing the experiments and interpreting the data. C.T.B. designed the study, analyzed data, funded the study, and drafted the manuscript. All authors contributed to the writing of the manuscript. Acknowledgement This work was supported by the Margot and Erich Goldschmidt & Peter René Jacobson-Stiftung and the Swiss National Science Foundation (SNSF; grant 310030_192440 to C.T.B.). 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Supplementary Files R1NPJHirisgerADCPandheatSupplMatCLEAN.pdf Cite Share Download PDF Status: Published Journal Publication published 02 May, 2026 Read the published version in npj Vaccines → Version 1 posted Editorial decision: Revision requested 13 Apr, 2026 Reviews received at journal 12 Apr, 2026 Reviews received at journal 11 Apr, 2026 Reviews received at journal 06 Apr, 2026 Reviews received at journal 01 Apr, 2026 Reviews received at journal 30 Mar, 2026 Reviewers agreed at journal 29 Mar, 2026 Reviewers agreed at journal 28 Mar, 2026 Reviewers agreed at journal 28 Mar, 2026 Reviewers agreed at journal 27 Mar, 2026 Reviewers agreed at journal 26 Mar, 2026 Reviewers invited by journal 26 Mar, 2026 Submission checks completed at journal 26 Mar, 2026 First submitted to journal 10 Mar, 2026 You are reading this latest preprint version Research Square lets you share your work early, gain feedback from the community, and start making changes to your manuscript prior to peer review in a journal. As a division of Research Square Company, we’re committed to making research communication faster, fairer, and more useful. We do this by developing innovative software and high quality services for the global research community. Our growing team is made up of researchers and industry professionals working together to solve the most critical problems facing scientific publishing. Also discoverable on Platform About Our Team In Review Editorial Policies Advisory Board Help Center Resources Author Services Accessibility API Access RSS feed Manage Cookie Preferences © Research Square 2026 | ISSN 2693-5015 (online) Privacy Policy Terms of Service Do Not Sell My Personal Information {"props":{"pageProps":{"initialData":{"identity":"rs-8338543","acceptedTermsAndConditions":true,"allowDirectSubmit":false,"archivedVersions":[],"articleType":"Article","associatedPublications":[],"authors":[{"id":613923296,"identity":"26d5b302-ccc7-4a0b-9e1d-68d9ed407d5f","order_by":0,"name":"Julia R. Hirsiger","email":"","orcid":"","institution":"University of Basel","correspondingAuthor":false,"prefix":"","firstName":"Julia","middleName":"R.","lastName":"Hirsiger","suffix":""},{"id":613923297,"identity":"93f705fd-1ae6-4906-979b-17b97c149d93","order_by":1,"name":"Silke Scarascia","email":"","orcid":"","institution":"University Hospital Basel","correspondingAuthor":false,"prefix":"","firstName":"Silke","middleName":"","lastName":"Scarascia","suffix":""},{"id":613923298,"identity":"963c3485-c27b-40e3-a0c3-95c28c107d79","order_by":2,"name":"Mike Recher","email":"","orcid":"","institution":"University Hospital Basel","correspondingAuthor":false,"prefix":"","firstName":"Mike","middleName":"","lastName":"Recher","suffix":""},{"id":613923299,"identity":"9adb83d8-d6bc-40a2-ae64-2d6fe7f67eda","order_by":3,"name":"Glenn Bantug","email":"","orcid":"","institution":"University of Basel","correspondingAuthor":false,"prefix":"","firstName":"Glenn","middleName":"","lastName":"Bantug","suffix":""},{"id":613923300,"identity":"04a96825-fe1b-44d3-ba38-94c4a419b690","order_by":4,"name":"Christoph T. Berger","email":"data:image/png;base64,iVBORw0KGgoAAAANSUhEUgAAAZAAAAAyAQMAAABI0h/eAAAABlBMVEX///8AAABVwtN+AAAACXBIWXMAAA7EAAAOxAGVKw4bAAAA+0lEQVRIiWNgGAWjYDACCQaGAyDagIEHIsDPwMDGABXEoyUBSYtkAxFaGFC0GBwgoIV/du/Dgz9/2OSZM/AefFzxyybf+Eb6swcMNXdwW3LnuMFhnoS0YssGvmTDs31plttu5JgbMBx7hlOLgUQaw2GGhMOJGw7wmEk29hw2MLuRwybB2HAYr5aDPyBazH829vw3MJ6R/oyglgM8UFsYG34cMDCQSDDDq0XiBtBhPGlpxQaH+ZIlGxuSDSTOvDE3SDiGWwv/jDTmjz9sbPIMjvce/Njwx86Avx0YYh9qcGuBgQQGZiDJ2AbnEgZQNX+IUDoKRsEoGAUjDgAALUZa51uVU6cAAAAASUVORK5CYII=","orcid":"","institution":"University of Basel","correspondingAuthor":true,"prefix":"","firstName":"Christoph","middleName":"T.","lastName":"Berger","suffix":""}],"badges":[],"createdAt":"2025-12-11 16:08:17","currentVersionCode":1,"declarations":"","doi":"10.21203/rs.3.rs-8338543/v1","doiUrl":"https://doi.org/10.21203/rs.3.rs-8338543/v1","draftVersion":[],"editorialEvents":[{"content":"https://doi.org/10.1038/s41541-026-01477-x","type":"published","date":"2026-05-02T15:58:33+00:00"}],"editorialNote":"","failedWorkflow":false,"files":[{"id":105845412,"identity":"d4c7e35e-9486-4a27-a104-64d73d993c4c","added_by":"auto","created_at":"2026-03-31 17:43:31","extension":"png","order_by":1,"title":"Figure 1","display":"","copyAsset":false,"role":"figure","size":330236,"visible":true,"origin":"","legend":"\u003cp\u003eFcγR-mediated monocyte activation by HA-IgG immune complexes. (A) C1q binding of HA-IgG-IC formed by pre-vaccination sera of ΔT\u003csup\u003ehi\u003c/sup\u003e (n=11) and ΔT\u003csup\u003elo\u003c/sup\u003e (N=27) subjects. Data are presented as median ± IQR. (B) ELISA-based measurement of C4d deposition on HA–IgG-IC formed with pre-vaccination sera from ΔT\u003csup\u003ehi\u003c/sup\u003e (n=11) and ΔT\u003csup\u003elo\u003c/sup\u003e subjects (n=27) to assess activation of the classical complement pathway. (C) Comparison of spontaneous, ADCP-mediated, and TLR-stimulated HA phagocytosis in ΔT\u003csup\u003ehi\u003c/sup\u003e vs. ΔT\u003csup\u003elo\u003c/sup\u003e monocytes. Pooled data of n= 3 independent experiments with two donors per group and experiment (n=6 ΔT\u003csup\u003elo\u003c/sup\u003e, n=6 ΔT\u003csup\u003ehi\u003c/sup\u003e). Data are presented as median ± IQR (A-C). (D) Heatmap summarizing immune complex-mediated activation (CD86/HLA-DR), cytokine (IL-6/IL-1) secretion, and antibody-dependent phagocytosis (ADCP) in the THP-1 monocyte cell line incubated with sera or HA-IC from ΔT\u003csup\u003ehi\u003c/sup\u003e (n=11) and ΔT\u003csup\u003elo\u003c/sup\u003e subjects (n=27). Color scale represents vector-scaled values, obtained by dividing each value by its Euclidean norm (√∑x²). nil= unstimulated THP-1, HA= hemagglutinin alone. (E) Example temperature curve (left) and summary graph (right) of cellular heat production following IC-mediated activation in THP-1 cell cultures measured using a thermal probe. Pooled data of n= 5 independent experiments with two donors per experiment (n=5 ΔT\u003csup\u003elo\u003c/sup\u003e, n=5 ΔT\u003csup\u003ehi\u003c/sup\u003e). (F) Immunofluorescence microscopy using the thermo-sensitive MTY on ΔT\u003csup\u003ehi\u003c/sup\u003e vs. ΔT\u003csup\u003elo\u003c/sup\u003e HA-IgG-IC activated THP-1 (left) and summary graph (right). Pooled data of n= 3 independent experiments with two donors per group and experiment (n=6 ΔT\u003csup\u003elo\u003c/sup\u003e, n=6 ΔT\u003csup\u003ehi\u003c/sup\u003e). Data are presented as median ± IQR (F, G). Statistical comparisons were performed using Mann-Whitney \u003cem\u003eU\u003c/em\u003e tests and one-way ANOVA with Dunn’s multiple comparison test as appropriate. *\u003cem\u003ep\u003c/em\u003e\u0026lt;0.05, **p\u0026lt;0.01, ****p\u0026lt;0.0001. HA-IC= immunocomplexes formed from recombinant hemagglutinin and serum IgG. QIV= quadrivalent influenza vaccine. LPS= lipopolysaccharide (TLR4 agonist), °C= degrees Celsius, MTY= MitoThermo Yellow.\u003c/p\u003e","description":"","filename":"OnlineFigure3.png","url":"https://assets-eu.researchsquare.com/files/rs-8338543/v1/61d3cd686a801d16fa6b70d7.png"},{"id":105904666,"identity":"70f5b759-4ed3-4b8e-be84-630970f54763","added_by":"auto","created_at":"2026-04-01 10:10:09","extension":"png","order_by":2,"title":"Figure 2","display":"","copyAsset":false,"role":"figure","size":290366,"visible":true,"origin":"","legend":"\u003cp\u003eAssociation of pre-vaccination immune profiles with thermal local reactions. (A) A visual demarcation of the ΔT threshold (n=38) at 1°C (dashed line) to divide the cohort into individuals with elevated temperature responses (ΔT\u003csup\u003ehi\u003c/sup\u003e) compared to those with a mild thermal reaction (ΔT\u003csup\u003elo\u003c/sup\u003e). (B) Influenza-specific T cell response measured by IFNg-Elispot (SFU/M = spot-forming units per million PBMC). (C) Pre-vaccination hemagglutinin-strain-specific IgG in Luminex and (D) neutralization titer in HA-inhibition assays. (E) Binding affinity measured by biolayer interferometry (BLI) against H1 and H3 expressed as equilibrium dissociation constant (KD) in Molar (M). Data are presented as median ± IQR (A-E) with n=27 for ΔT\u003csup\u003elo \u003c/sup\u003eand n=11 for ΔT\u003csup\u003ehi\u003c/sup\u003e in all experiments. (F) IgG, IgA, IgM, and IgG\u003csub\u003e1-4\u003c/sub\u003e subclass contributions to the HA-binding antibodies are expressed as the median ratio ΔT\u003csup\u003ehi\u003c/sup\u003e / ΔT\u003csup\u003elo\u003c/sup\u003e ± upper/ lower limits (i.e., values \u0026gt;1 indicate higher antibody levels of this subclass in ΔT\u003csup\u003ehi\u003c/sup\u003e). n=27 for ΔT\u003csup\u003elo \u003c/sup\u003eand n=11 for ΔT\u003csup\u003ehi\u003c/sup\u003e. (G) Correlation of HA-specific IgG1 levels with ΔT in absolute values (n=38) by simple linear regression analysis. The p and r values were obtained using Pearson correlation. °C= degrees Celsius, H1= hemagglutinin from H1N1 vaccine strain; H3= hemagglutinin from H3N2 vaccine strain. QIV= quadrivalent influenza vaccine. MFI= median fluorescence intensity. BL= baseline. Statistical comparisons were performed using Mann-Whitney \u003cem\u003eU\u003c/em\u003e tests. *\u003cem\u003ep\u003c/em\u003e\u0026lt;0.05, **\u003cem\u003ep\u003c/em\u003e\u0026lt;0.01, ***p\u0026lt;0.001\u003c/p\u003e","description":"","filename":"OnlineFigure2.png","url":"https://assets-eu.researchsquare.com/files/rs-8338543/v1/2ec6d50bfad4dca3517a6649.png"},{"id":105845414,"identity":"3f7782f9-87e7-4ec3-ada0-830c94de54b4","added_by":"auto","created_at":"2026-03-31 17:43:31","extension":"png","order_by":3,"title":"Figure 3","display":"","copyAsset":false,"role":"figure","size":239232,"visible":true,"origin":"","legend":"\u003cp\u003eClinical correlates of the local thermal reactogenicity. (A) Schematic of systemic (temporal) and local (deltoid) temperature measurements. (B) Systemic temperature (in °C) measured before (0h) and 24h post-vaccination (24h) at the left (L) and right (R) temporal regions. (C) Local temperatures at the unvaccinated (control) and vaccinated (vaccine) arms are indicated at the pre- (n=34) and 24h post-vaccination (n=38) time points. Box plots display the median and 25\u003csup\u003eth\u003c/sup\u003e-75\u003csup\u003eth\u003c/sup\u003e percentiles and whiskers the 10\u003csup\u003eth\u003c/sup\u003e-90\u003csup\u003eth \u003c/sup\u003epercentiles. Local temperature reactions (median and interquartile range) stratified by (D) sex, (E) presence of erythema, (F) pain, and (G) the number of prior vaccinations in the last five years. Statistical comparisons were performed using Wilcoxon signed-rank or Mann-Whitney \u003cem\u003eU\u003c/em\u003e tests as appropriate. *\u003cem\u003ep\u003c/em\u003e\u0026lt;0.05, ****p\u0026lt;0.0001. QIV= quadrivalent influenza vaccine; °C= degrees Celsius, T\u003csub\u003esys\u003c/sub\u003e= systemic temperature, T\u003csub\u003evacc\u003c/sub\u003e= temperature at the vaccinated arm, T\u003csub\u003ectrl\u003c/sub\u003e= temperature at the control arm. M= men, F= women.\u003c/p\u003e","description":"","filename":"OnlineFigure1.png","url":"https://assets-eu.researchsquare.com/files/rs-8338543/v1/32213fe8623bbc94cc6823a4.png"},{"id":105845416,"identity":"8fa04a66-da3d-466c-a165-97e40692ee81","added_by":"auto","created_at":"2026-03-31 17:43:31","extension":"png","order_by":4,"title":"Figure 4","display":"","copyAsset":false,"role":"figure","size":356921,"visible":true,"origin":"","legend":"\u003cp\u003eEffect of temperature on B cell function. (A) \u003cem\u003eIn vitro\u003c/em\u003e plasmablast differentiation (example FACS plot and summary graph) and (B) B cell proliferation (example CTV dilution histogram and summary graph) after PBMC stimulation with QIV at a cell culture temperature of 37°C (grey) vs. 39°C (purple). Frequency of PB (CD3\u003csup\u003e-\u003c/sup\u003eCD19\u003csup\u003e+\u003c/sup\u003eCD20\u003csup\u003e-\u003c/sup\u003eCD27\u003csup\u003e+\u003c/sup\u003eCD38\u003csup\u003e+\u003c/sup\u003e) and proliferated B cells (CTV\u003csup\u003elow\u003c/sup\u003e) after five days is shown. (C) Total IgG production (ELISA) and (D) A/Kansas/14/2017 (H3N2)-specific IgG production (Luminex) were compared at 37°C vs 39°C. (E) The avidity of A/Kansas/14/2017 (H3N2)-specific IgG produced at 37°C vs. 39°C was compared in urea challenge assays. Data represent three independent experiments, each with three different donors (n=9). Data are presented as median ± IQR. Statistical comparisons were performed using Mann-Whitney \u003cem\u003eU\u003c/em\u003e tests **p\u0026lt;0.01. PB= plasmablasts, QIV= quadrivalent influenza vaccine, CTV= CellTrace™ Violet, °C= degrees Celsius.\u003c/p\u003e","description":"","filename":"OnlineFigure4.png","url":"https://assets-eu.researchsquare.com/files/rs-8338543/v1/3d7cd1bbcb96b864de12fb74.png"},{"id":105905197,"identity":"6d66e292-61d4-4831-8804-23fd556460d7","added_by":"auto","created_at":"2026-04-01 10:11:35","extension":"png","order_by":5,"title":"Figure 5","display":"","copyAsset":false,"role":"figure","size":341777,"visible":true,"origin":"","legend":"\u003cp\u003e\u003cem\u003eIn vivo\u003c/em\u003e associations of local temperature reactogenicity and the adaptive vaccine response. (A) Unsupervised hierarchical clustering analysis of baseline immune profiles and the vaccine response outcomes. (B) Peripheral blood frequencies of Tfh and (C) PB seven days post-vaccination. (D) QIV- and HA-specific T cell responses at day 28 in IFNg EliSpot expressed as SFC/M. (E) Hemagglutinin-specific IgG levels post-vaccination in strain-specific Luminex. (F) Neutralization titers in HA inhibition assays against the vaccine strains A/Brisbane/02/2018 (H1N1) and A/Kansas/14/2017 (H3N2). The dashed line indicates the seroprotective titer 1:40. (G) Antibody avidity in biolayer interferometry expressed as KD. Data are presented as median ± IQR in A-F (n=11 DT\u003csup\u003ehi\u003c/sup\u003e, n=27 DT\u003csup\u003elo\u003c/sup\u003e). (H) Heatmap of non-neutralizing, Fc-mediated antibody functions tested using HA-IgG-IC formed from serum day 28 post-vaccination. Color scale represents vector-scaled values (n=5 DT\u003csup\u003ehi\u003c/sup\u003e, n=5 DT\u003csup\u003elo\u003c/sup\u003e), obtained by dividing each value by their Euclidean norm (√∑x²). Statistical comparisons were performed using Mann-Whitney U tests. *\u003cem\u003ep\u003c/em\u003e\u0026lt;0.05, **p\u0026lt;0.01, ****p\u0026lt;0.0001. Tfh= circulating follicular T helper-like T cells, PB= plasmablasts, SFC/M = spot-forming cells per million PBMC, HA-IC= recombinant hemagglutinin/serum IgG-immunocomplexes.\u003c/p\u003e","description":"","filename":"OnlineFigure5.png","url":"https://assets-eu.researchsquare.com/files/rs-8338543/v1/5fc642dd3ca98d2f2790b6fc.png"},{"id":108495216,"identity":"187054d5-5f89-43e2-9678-776e7393cade","added_by":"auto","created_at":"2026-05-05 10:09:21","extension":"pdf","order_by":0,"title":"","display":"","copyAsset":false,"role":"manuscript-pdf","size":2941580,"visible":true,"origin":"","legend":"","description":"","filename":"manuscript.pdf","url":"https://assets-eu.researchsquare.com/files/rs-8338543/v1/1bca20f5-7dd2-4d18-b87e-ef271cd08f50.pdf"},{"id":105904581,"identity":"b540f4de-d3ab-4792-8cc6-b2b56ff5c5eb","added_by":"auto","created_at":"2026-04-01 10:09:43","extension":"pdf","order_by":1,"title":"","display":"","copyAsset":false,"role":"supplement","size":12289483,"visible":true,"origin":"","legend":"","description":"","filename":"R1NPJHirisgerADCPandheatSupplMatCLEAN.pdf","url":"https://assets-eu.researchsquare.com/files/rs-8338543/v1/a6b8138425fbabeca57492eb.pdf"}],"financialInterests":"Competing interest reported. The Authors declare no competing financial or non-financial interest in relation to the study. C.T.B. is chair of the Swiss National Immunization Technical Advisory Group (NITAG).","formattedTitle":"Preexisting IgG forms immune complexes and links local thermal reactogenicity with immunogenicity in influenza vaccination","fulltext":[{"header":"Introduction","content":"\u003cp\u003eVaccination induces a pathogen-specific immune response to prevent subsequent infections. Protection is conferred by humoral B cell and T cell responses. Vaccine-specific B cells emerge from both follicular and extrafollicular pathways, leading to the development of either long-lived plasma cells and memory B cells, or short-lived antibody-secreting cells that provide rapid, yet temporary, immunological protection\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e1\u003c/span\u003e\u003c/sup\u003e. The determination of B cell response fate, whether follicular or extrafollicular, depends on the antigen type, T cell help, cytokine environment, and pre-existing memory from prior antigen exposure\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e1\u003c/span\u003e,\u003cspan class=\"CitationRef\"\u003e2\u003c/span\u003e\u003c/sup\u003e. Generally, primary immune responses are characterized by extrafollicular plasmablasts that produce low-affinity antibodies, while some B cells migrate to germinal centers to undergo affinity maturation. Secondary responses involve follicular memory B cells that rapidly differentiate into plasma cells producing higher-affinity antibodies\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e3\u003c/span\u003e,\u003cspan class=\"CitationRef\"\u003e4\u003c/span\u003e\u003c/sup\u003e. Humans are frequently exposed to respiratory viruses. For influenza, it is estimated that most individuals become infected at least once over six seasons\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e5\u003c/span\u003e\u003c/sup\u003e. Therefore, the seasonal influenza vaccine encounters a primed immune system with pre-existing antigen-specific antibodies and memory B cells\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e6\u003c/span\u003e\u003c/sup\u003e. Importantly, humoral responses to influenza vaccination can be diminished or enhanced by pre-existing immunity, depending on the antigen and the functional characteristics of the pre-existing humoral immunity\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e6\u003c/span\u003e\u003c/sup\u003e.\u003c/p\u003e \u003cp\u003eWhile antibody-mediated protective immunity is primarily provided by neutralizing antibodies that block the virus from infecting cells\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e1\u003c/span\u003e\u003c/sup\u003e, it became evident that non-neutralizing antibodies exert various protective or modulatory functions in the vaccine response\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e7\u003c/span\u003e\u003c/sup\u003e. Through Fc-dependent pathways, such as antibody-dependent cellular phagocytosis (ADCP), cellular cytotoxicity (ADCC) or through complement activation (ADCA), these antibodies can label virions for uptake, shape antigen processing, and influence downstream adaptive responses\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e7\u003c/span\u003e,\u003cspan class=\"CitationRef\"\u003e8\u003c/span\u003e\u003c/sup\u003e. There is increasing evidence that non-neutralizing anti-hemagglutinin (HA) antibodies contribute to influenza vaccine-induced protection\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e9\u003c/span\u003e–\u003cspan class=\"CitationRef\"\u003e11\u003c/span\u003e\u003c/sup\u003e. In natural infections and immunizations with replication-competent viruses (e.g., vector or live attenuated vaccines), pre-existing immunity accelerates viral or vaccine virus clearance and can, in rare cases, facilitate antibody-dependent disease enhancement\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e12\u003c/span\u003e,\u003cspan class=\"CitationRef\"\u003e13\u003c/span\u003e\u003c/sup\u003e. In contrast, vaccinations containing viral protein antigens rely on a high amount of antigen to surpass the antigenic threshold for effective immune priming\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e14\u003c/span\u003e\u003c/sup\u003e. FcR-dependent interactions of serum IgG with a protein antigen have been described, including the formation of immune complexes\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e15\u003c/span\u003e,\u003cspan class=\"CitationRef\"\u003e16\u003c/span\u003e\u003c/sup\u003e. However, the extent to which distinct pre-existing anti-influenza antibody profiles can influence vaccine antigen uptake via Fc-mediated functions and, subsequently, the induction of the adaptive immune response to influenza vaccination, is poorly understood. Furthermore, how antibody-Fc-receptor-mediated pathways of innate immune activation contribute to reactogenicity has not been thoroughly examined.\u003c/p\u003e \u003cp\u003eLocal injection site reactions (ISR) are the most common adverse events following immunization. The local inflammation associated with ISR is mediated by innate immune activation; a crucial element in initiating the immune response to vaccines. Vaccine-mediated activation of pathogen- or damage-associated molecular patterns (PAMPs and DAMPs) leads to the release of pro-inflammatory cytokines, cell migration and antigen uptake via endocytosis or phagocytosis\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e17\u003c/span\u003e\u003c/sup\u003e. Local inflammation arises a few hours after vaccination and usually resolves within three days\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e17\u003c/span\u003e\u003c/sup\u003e. Pre-existing vaccine-specific immunity contributes to the vaccine reactogenicity, as evidenced by severe local reactions (‘hyperimmunization’)\u003csup\u003e18\u003c/sup\u003e or immune-complex-mediated reactions (Arthus reactions or type III hypersensitivity reactions)\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e19\u003c/span\u003e\u003c/sup\u003e. Few studies have investigated whether the reactogenicity of the influenza vaccine is associated with vaccine immunogenicity or efficacy. In heart failure patients, adverse events following influenza vaccination were associated with better cardiovascular outcomes\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e20\u003c/span\u003e\u003c/sup\u003e. A post-hoc analysis of an immunogenicity study observed stronger local reactions in subjects with low pre-existing immunity but a high antibody fold increase\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e21\u003c/span\u003e\u003c/sup\u003e. In studies of COVID-19 vaccines, fever, but not local reactogenicity, was associated with higher antibody levels\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e22\u003c/span\u003e–\u003cspan class=\"CitationRef\"\u003e25\u003c/span\u003e\u003c/sup\u003e. Notably, none of these studies monitored local temperature reactions.\u003c/p\u003e \u003cp\u003eHere, we studied the contributing immunological factors and consequences of local temperature reactions to seasonal influenza vaccination in a human model system with variable pre-existing immunity and reactogenicity.\u003c/p\u003e"},{"header":"Results","content":"\u003cdiv id=\"Sec3\" class=\"Section2\"\u003e \u003ch2\u003eInfluenza vaccination induced a local thermal reaction 24 hours post-vaccination\u003c/h2\u003e \u003cp\u003eBetween November 2019 and January 2020, 38 healthy subjects who received the inactivated seasonal influenza vaccination were enrolled. The baseline characteristics of the study population are summarized in Table\u0026nbsp;\u003cspan refid=\"Tab1\" class=\"InternalRef\"\u003e1\u003c/span\u003e. We measured temperatures at the temporal region (\u0026lsquo;systemic temperature\u0026rsquo;) and the deltoid region (\u0026lsquo;injection site\u0026rsquo; and \u0026rsquo;control site\u0026rsquo;) before and 24 hours following quadrivalent inactivated influenza vaccination (QIV) using a no-touch temporal thermometer (Fig.\u0026nbsp;\u003cspan refid=\"Fig1\" class=\"InternalRef\"\u003e1\u003c/span\u003eA). The increase in skin surface temperature at the injection site was defined as the \u0026lsquo;local thermal reaction/reactogenicity\u0026rsquo;. Systemic temperature was unchanged 24h post-vaccination and comparable between the two temporal measurement sites (baseline median T\u003csub\u003etemp(L)\u003c/sub\u003e 36.85\u0026deg;C vs. T\u003csub\u003etemp(R)\u003c/sub\u003e 36.80\u0026deg;C, p\u0026thinsp;=\u0026thinsp;0.90; 24h post-vaccination median T\u003csub\u003etemp(L)\u003c/sub\u003e 36.83\u0026deg;C vs. T\u003csub\u003etemp(R)\u003c/sub\u003e 36.88\u0026deg;C, p\u0026thinsp;=\u0026thinsp;0.98) (Fig.\u0026nbsp;\u003cspan refid=\"Fig1\" class=\"InternalRef\"\u003e1\u003c/span\u003eB). Vaccination induced a significant temperature increase at the vaccinated arm 24h post-vaccination (median T\u003csub\u003evacc\u003c/sub\u003e 36.63\u0026deg;C vs. 35.90\u0026deg;C; p\u0026thinsp;\u0026lt;\u0026thinsp;0.0001) but not at the control arm (median T\u003csub\u003ectrl\u003c/sub\u003e 36.05\u0026deg;C vs. 35.95\u0026deg;C; p\u0026thinsp;=\u0026thinsp;0.73) (Fig.\u0026nbsp;\u003cspan refid=\"Fig1\" class=\"InternalRef\"\u003e1\u003c/span\u003eC). The median temperature increase at the vaccinated arm was higher in women (ΔT\u003csub\u003evacc24h\u0026minus;BL\u003c/sub\u003e +0.63\u0026deg;C vs. +0.32\u0026deg;C in men, p\u0026thinsp;=\u0026thinsp;0.04) (Fig.\u0026nbsp;\u003cspan refid=\"Fig1\" class=\"InternalRef\"\u003e1\u003c/span\u003eD) and in those with a clinically observed local erythema (ΔT\u003csub\u003evacc24h\u0026minus;BL\u003c/sub\u003e +1.55 vs. +0.35\u0026deg;C, p\u0026thinsp;\u0026lt;\u0026thinsp;0.0001) (Fig.\u0026nbsp;\u003cspan refid=\"Fig1\" class=\"InternalRef\"\u003e1\u003c/span\u003eE). The erythema diameter was correlated with the ΔT at the vaccine arm (\u003cb\u003eSupplementary Fig.\u0026nbsp;3, p\u003c/b\u003e\u0026thinsp;\u0026lt;\u0026thinsp;0.0001, r\u0026thinsp;=\u0026thinsp;0.68), and self-reported severe pain showed a significant correlation with the temperature increase (Fig.\u0026nbsp;\u003cspan refid=\"Fig1\" class=\"InternalRef\"\u003e1\u003c/span\u003eF\u003cem\u003e)\u003c/em\u003e. The number of influenza vaccines received in the preceding five years had no influence (Fig.\u0026nbsp;\u003cspan refid=\"Fig1\" class=\"InternalRef\"\u003e1\u003c/span\u003eG\u003cem\u003e).\u003c/em\u003e\u003c/p\u003e \u003cp\u003e \u003cdiv class=\"gridtable\"\u003e\u003ctable float=\"Yes\" id=\"Tab1\" border=\"1\"\u003e \u003ccaption language=\"En\"\u003e \u003cdiv class=\"CaptionNumber\"\u003eTable 1\u003c/div\u003e \u003cdiv class=\"CaptionContent\"\u003e \u003cp\u003eBaseline Characteristics\u003c/p\u003e \u003c/div\u003e \u003c/caption\u003e \u003ccolgroup cols=\"2\"\u003e \u003cdiv align=\"left\" class=\"colspec\" colname=\"c1\" colnum=\"1\"\u003e\u003c/div\u003e \u003cdiv align=\"char\" char=\".\" class=\"colspec\" colname=\"c2\" colnum=\"2\"\u003e\u003c/div\u003e \u003cthead\u003e \u003ctr\u003e \u003cth align=\"left\" colname=\"c1\"\u003e \u003cp\u003eTotal\u003c/p\u003e \u003c/th\u003e \u003cth align=\"left\" colname=\"c2\"\u003e \u003cp\u003en\u0026thinsp;=\u0026thinsp;38\u003c/p\u003e \u003c/th\u003e \u003c/tr\u003e \u003c/thead\u003e \u003ctbody\u003e \u003ctr\u003e \u003ctd align=\"left\" colname=\"c1\"\u003e \u003cp\u003eWomen, n (%)\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c2\"\u003e \u003cp\u003e27 (70.5%)\u003c/p\u003e \u003c/td\u003e \u003c/tr\u003e \u003ctr\u003e \u003ctd align=\"left\" colname=\"c1\"\u003e \u003cp\u003eAge, median (IQR)\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c2\"\u003e \u003cp\u003e31 (27-42.5)\u003c/p\u003e \u003c/td\u003e \u003c/tr\u003e \u003ctr\u003e \u003ctd align=\"left\" colname=\"c1\"\u003e \u003cp\u003eBMI, median (range)\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c2\"\u003e \u003cp\u003e21.9 (20.7\u0026ndash;24.1)\u003c/p\u003e \u003c/td\u003e \u003c/tr\u003e \u003ctr\u003e \u003ctd align=\"left\" colname=\"c1\"\u003e \u003cp\u003eVaccinated arm\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"left\" colname=\"c2\"\u003e\u0026nbsp;\u003c/td\u003e \u003c/tr\u003e \u003ctr\u003e \u003ctd align=\"left\" colname=\"c1\"\u003e \u003cp\u003e- left\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c2\"\u003e \u003cp\u003e34 (89.5%)\u003c/p\u003e \u003c/td\u003e \u003c/tr\u003e \u003ctr\u003e \u003ctd align=\"left\" colname=\"c1\"\u003e \u003cp\u003e- right\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c2\"\u003e \u003cp\u003e4 (10.5%)\u003c/p\u003e \u003c/td\u003e \u003c/tr\u003e \u003ctr\u003e \u003ctd align=\"left\" colname=\"c1\"\u003e \u003cp\u003eMedical history\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"left\" colname=\"c2\"\u003e\u0026nbsp;\u003c/td\u003e \u003c/tr\u003e \u003ctr\u003e \u003ctd align=\"left\" colname=\"c1\"\u003e \u003cp\u003e- Allergy*\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c2\"\u003e \u003cp\u003e15 (39.5%)\u003c/p\u003e \u003c/td\u003e \u003c/tr\u003e \u003ctr\u003e \u003ctd align=\"left\" colname=\"c1\"\u003e \u003cp\u003e- Autoimmunity**\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c2\"\u003e \u003cp\u003e3 (7.9%)\u003c/p\u003e \u003c/td\u003e \u003c/tr\u003e \u003ctr\u003e \u003ctd align=\"left\" colname=\"c1\"\u003e \u003cp\u003e- Current Smoker\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c2\"\u003e \u003cp\u003e1 (2.6%)\u003c/p\u003e \u003c/td\u003e \u003c/tr\u003e \u003ctr\u003e \u003ctd align=\"left\" colname=\"c1\"\u003e \u003cp\u003eILI past 5 years\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"left\" colname=\"c2\"\u003e\u0026nbsp;\u003c/td\u003e \u003c/tr\u003e \u003ctr\u003e \u003ctd align=\"left\" colname=\"c1\"\u003e \u003cp\u003e- none\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c2\"\u003e \u003cp\u003e27 (70.5%)\u003c/p\u003e \u003c/td\u003e \u003c/tr\u003e \u003ctr\u003e \u003ctd align=\"left\" colname=\"c1\"\u003e \u003cp\u003e- previous year only\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c2\"\u003e \u003cp\u003e1 (2.6%)\u003c/p\u003e \u003c/td\u003e \u003c/tr\u003e \u003ctr\u003e \u003ctd align=\"left\" colname=\"c1\"\u003e \u003cp\u003e- \u0026gt;\u0026thinsp;1\u0026ndash;5 years ago\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c2\"\u003e \u003cp\u003e10 (26.3%)\u003c/p\u003e \u003c/td\u003e \u003c/tr\u003e \u003ctr\u003e \u003ctd align=\"left\" colname=\"c1\"\u003e \u003cp\u003eInfluenza vaccines (past 5 years)\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"left\" colname=\"c2\"\u003e\u0026nbsp;\u003c/td\u003e \u003c/tr\u003e \u003ctr\u003e \u003ctd align=\"left\" colname=\"c1\"\u003e \u003cp\u003e- 0\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c2\"\u003e \u003cp\u003e11 (28.9%)\u003c/p\u003e \u003c/td\u003e \u003c/tr\u003e \u003ctr\u003e \u003ctd align=\"left\" colname=\"c1\"\u003e \u003cp\u003e- 1\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c2\"\u003e \u003cp\u003e11 (28.9%)\u003c/p\u003e \u003c/td\u003e \u003c/tr\u003e \u003ctr\u003e \u003ctd align=\"left\" colname=\"c1\"\u003e \u003cp\u003e- 2\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c2\"\u003e \u003cp\u003e2 (5.3%)\u003c/p\u003e \u003c/td\u003e \u003c/tr\u003e \u003ctr\u003e \u003ctd align=\"left\" colname=\"c1\"\u003e \u003cp\u003e- 3\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c2\"\u003e \u003cp\u003e4 (10.5%)\u003c/p\u003e \u003c/td\u003e \u003c/tr\u003e \u003ctr\u003e \u003ctd align=\"left\" colname=\"c1\"\u003e \u003cp\u003e- 4\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c2\"\u003e \u003cp\u003e3 (7.9%)\u003c/p\u003e \u003c/td\u003e \u003c/tr\u003e \u003ctr\u003e \u003ctd align=\"left\" colname=\"c1\"\u003e \u003cp\u003e- 5\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c2\"\u003e \u003cp\u003e7 (18.4%)\u003c/p\u003e \u003c/td\u003e \u003c/tr\u003e \u003c/tbody\u003e \u003c/colgroup\u003e \u003ctfoot\u003e \u003ctr\u003e\u003ctd colspan=\"2\"\u003e*RCA=allergic rhinoconjunctivitis, asthma, penicillin; **Basedow (n\u0026thinsp;=\u0026thinsp;1), Psoriasis(n\u0026thinsp;=\u0026thinsp;2); ILI= influenza like illness\u003c/td\u003e\u003c/tr\u003e \u003c/tfoot\u003e \u003c/table\u003e\u003c/div\u003e \u003c/p\u003e \u003cp\u003e \u003c/p\u003e \u003c/div\u003e\n\u003ch3\u003ePre-existing IgGs from subjects with subsequently augmented thermal reactogenicity potently activated monocytes\u003c/h3\u003e\n\u003cp\u003eLocal injection-site reactions result from vaccine- or adjuvant-mediated innate immune activation. Immune complexes can trigger cytokine-independent monocyte activation via the Fc-receptor (FcR) or complement receptors. IgG1, the HA-specific IgG subclass that was significantly elevated in pre-immunization sera of ΔT\u003csup\u003ehi\u003c/sup\u003e subjects, potently activates FcR\u003csup\u003e\u003cspan citationid=\"CR27\" class=\"CitationRef\"\u003e27\u003c/span\u003e\u003c/sup\u003e. Accordingly, we examined whether the higher levels of anti-HA-IgG1 in ΔT\u003csup\u003ehi\u003c/sup\u003e subjects were associated with enhanced FcR-mediated monocyte activation or complement system activation. To test this, recombinant hemagglutinin was mixed with pre-vaccination sera to form HA-IgG immune complexes (HA-IgG-IC). Using a C1q-binding assay, we demonstrated that HA-IgG-IC from ΔT\u003csup\u003ehi\u003c/sup\u003e more robustly bound complement (Fig.\u0026nbsp;\u003cspan refid=\"Fig3\" class=\"InternalRef\"\u003e3\u003c/span\u003eA), which was directly correlated with the amount of HA-specific IgG (H1: r\u0026thinsp;=\u0026thinsp;0.73, p\u0026thinsp;\u0026lt;\u0026thinsp;0.0001; H3: r\u0026thinsp;=\u0026thinsp;0.72, p\u0026thinsp;\u0026lt;\u0026thinsp;0.0001). Next, we used an \u003cem\u003ein vitro\u003c/em\u003e complement activation assay that measures CD4d deposition by ELISA\u003csup\u003e\u003cspan citationid=\"CR28\" class=\"CitationRef\"\u003e28\u003c/span\u003e\u003c/sup\u003e. HA-IgG-IC from ΔT\u003csup\u003ehi\u003c/sup\u003e showed significantly stronger serum complement activation than HA-IgG-IC from ΔT\u003csup\u003elo\u003c/sup\u003e (Fig.\u0026nbsp;\u003cspan refid=\"Fig3\" class=\"InternalRef\"\u003e3\u003c/span\u003eB). The ADCP capacity of HA-IgG-IC formed with the pre-vaccination sera was assessed using fluorochrome-labeled hemagglutinin (HA\u003csub\u003efluo\u003c/sub\u003e) to monitor cellular uptake of HA\u003csub\u003efluo\u003c/sub\u003e-IgG-IC. Using primary monocytes and pre-vaccination sera from ΔT\u003csup\u003ehi\u003c/sup\u003e and ΔT\u003csup\u003elo\u003c/sup\u003e subjects, we observed an increased ADCP of HA\u003csub\u003efluo\u003c/sub\u003e-IgG-IC by monocytes from ΔT\u003csup\u003ehi\u003c/sup\u003e subjects (Fig.\u0026nbsp;\u003cspan refid=\"Fig3\" class=\"InternalRef\"\u003e3\u003c/span\u003eC). In contrast, there was no difference in HA uptake after FγR-independent monocyte activation by TLR4-stimulation with LPS, nor when the same experiments were conducted with mDCs (Fig.\u0026nbsp;\u003cspan refid=\"Fig3\" class=\"InternalRef\"\u003e3\u003c/span\u003eC, \u003cb\u003eSupplementary Fig.\u0026nbsp;7\u003c/b\u003e). We confirmed that IC uptake in this assay depended on a functional IgG/FcγR interaction using blocking antibodies against FcγRI (CD64), FcγRII (CD32), or FcγRIII (CD16), alone or in combination (\u003cb\u003eSupplementary Fig.\u0026nbsp;7\u003c/b\u003e). Overall, there was redundancy among the different FcγR, but blocking FcγRI most potently decreased IC phagocytosis. Complementary experiments using IgG-depleted sera or the serum of a subject with severe hypogammaglobulinemia further confirmed that HA uptake was mainly ADCP-mediated (\u003cb\u003eSupplementary Fig.\u0026nbsp;7\u003c/b\u003e).\u003c/p\u003e \u003cp\u003e \u003c/p\u003e \u003cp\u003eNext, we aimed to compare the ADCP function of the pre-vaccination sera in a controlled cellular system using the THP-1 cell line. Stimulation of the THP-1 monocyte cell line with pre-vaccination HA-IgG-IC from ΔT\u003csup\u003ehi\u003c/sup\u003e subjects induced significantly enhanced THP-1 activation (HLA-DR\u003csup\u003ehi\u003c/sup\u003e CD86\u003csup\u003ehi\u003c/sup\u003e), pro-inflammatory cytokine secretion (IL-1β and IL-6), and antibody-dependent phagocytosis (ADCP) compared to HA-IgG-IC from ΔT\u003csup\u003elo\u003c/sup\u003e subjects (Fig.\u0026nbsp;\u003cspan refid=\"Fig3\" class=\"InternalRef\"\u003e3\u003c/span\u003eD). The associations between the local thermal reaction and monocyte activation were comparable regardless of whether H3 or H1 was used as the hemagglutinin target (Fig.\u0026nbsp;\u003cspan refid=\"Fig3\" class=\"InternalRef\"\u003e3\u003c/span\u003eD \u003cb\u003eand Supplementary Fig.\u0026nbsp;8\u003c/b\u003e) and were confirmed using the absolute ΔT values in complementary correlation analyses (\u003cb\u003eSupplementary Fig.\u0026nbsp;8\u003c/b\u003e). ADCP and monocyte activation were closely connected to the levels of pre-existing HA-specific IgG1, the amount of HA-IgG-IC formed in vitro, and the clinically observed local thermal reactogenicity, which showed the strongest statistical correlation. (\u003cb\u003eSupplementary Figs.\u0026nbsp;9 and 10\u003c/b\u003e).\u003c/p\u003e \u003cp\u003e \u003cem\u003eIn vivo\u003c/em\u003e, we observed differences in the frequency of peripheral blood monocytes amongst PBMC 24 h post-vaccination in ΔT\u003csup\u003ehi\u003c/sup\u003e vs. ΔT\u003csup\u003elo\u003c/sup\u003e (median 10.0% vs. 17.7%, p\u0026thinsp;=\u0026thinsp;0.009), with lower frequencies of classical (CD14\u003csup\u003ehigh\u003c/sup\u003eCD16\u003csup\u003eneg\u003c/sup\u003e) monocytes (44.7% vs. 62.8%, p\u0026thinsp;=\u0026thinsp;0.004) and an increased frequency of non-classical (CD14\u003csup\u003elow\u003c/sup\u003eCD16\u003csup\u003ehigh\u003c/sup\u003e) monocytes (29.4% vs. 10.5%, p\u0026thinsp;=\u0026thinsp;0.041) in ΔT\u003csup\u003ehi\u003c/sup\u003e (\u003cb\u003eSupplementary Fig.\u0026nbsp;11\u003c/b\u003e\u003cem\u003e).\u003c/em\u003e These monocytes exhibited a higher median fluorescence intensity (MFI) of HLA-DR expression across all monocyte subsets (CD14\u003csup\u003ehigh\u003c/sup\u003eCD16\u003csup\u003enegative\u003c/sup\u003e, CD14\u003csup\u003ehigh\u003c/sup\u003eCD16\u003csup\u003elow\u003c/sup\u003e, and CD14\u003csup\u003elow\u003c/sup\u003eCD16\u003csup\u003ehigh\u003c/sup\u003e), while CD86 was only elevated on CD14\u003csup\u003ehigh\u003c/sup\u003eCD16\u003csup\u003enegative\u003c/sup\u003e monocytes (\u003cb\u003eSupplementary Fig.\u0026nbsp;11\u003c/b\u003e).\u003c/p\u003e \u003cp\u003eInflammation-related heat likely results from hyperemia driven by local cytokine release, but it may also stem from cellular heat generation. We investigated this by measuring the temperature of the cell culture media in stimulated THP-1 cells using an immersion temperature probe. Monocytes of ΔT\u003csup\u003ehi\u003c/sup\u003e subjects produced significantly more heat \u003cem\u003ein vitro\u003c/em\u003e (T 37.55\u0026deg;C vs. 37.76\u0026deg;C, p\u0026thinsp;=\u0026thinsp;0.0159) when activated by autologous HA-IgG-IC, but not when non-specifically activated with LPS (Fig.\u0026nbsp;\u003cspan refid=\"Fig3\" class=\"InternalRef\"\u003e3\u003c/span\u003eE,F). In addition, we employed a thermo-sensitive mitochondrial-targeted fluorescent dye, MitoThermo Yellow (MTY), to visualize mitochondrial temperature production at the cellular level in primary monocytes. In this assay, higher temperature production results in reduced MTY fluorescence intensity\u003csup\u003e\u003cspan citationid=\"CR29\" class=\"CitationRef\"\u003e29\u003c/span\u003e\u003c/sup\u003e. Differences in the mitochondrial temperature production were confirmed in the MTY assay comparing ΔT\u003csup\u003ehi\u003c/sup\u003e and ΔT\u003csup\u003elo\u003c/sup\u003e HA-IgG-IC-mediated THP-1 cell activation (MTY MFI 1058 vs. 2562, p\u0026thinsp;=\u0026thinsp;0.002) (Fig.\u0026nbsp;\u003cspan refid=\"Fig3\" class=\"InternalRef\"\u003e3\u003c/span\u003eG). Immune cell heat generation was almost exclusively monocyte-derived (\u003cb\u003eSupplementary Fig.\u0026nbsp;11\u003c/b\u003e).\u003c/p\u003e \u003cp\u003eTogether, these results suggest that higher anti-HA-IgG1 pre-vaccination levels may drive FcR-dependent or complement activation mediated monocyte activation through IC, resulting in more pronounced local thermal reactogenicity, potentially affected by increased heat generation of immune complex-activated innate immune cells.\u003c/p\u003e\n\u003ch3\u003eImpact of temperature on B cell functions in vitro\u003c/h3\u003e\n\u003cp\u003eThermal energy drives several immunological processes, including cell migration, cellular activation, cytokine secretion, and cell proliferation\u003csup\u003e\u003cspan additionalcitationids=\"CR31 CR32\" citationid=\"CR30\" class=\"CitationRef\"\u003e30\u003c/span\u003e\u0026ndash;\u003cspan citationid=\"CR33\" class=\"CitationRef\"\u003e33\u003c/span\u003e\u003c/sup\u003e. Although our data establish FcR-dependent monocyte heat generation \u003cem\u003ein vitro\u003c/em\u003e, the extent to which such micro-scale thermal changes occur \u003cem\u003ein vivo\u003c/em\u003e and reach the B cell niches remains to be defined. Nevertheless, these findings prompted us to examine how modest, transient temperature elevations might affect antigen-driven B cell activation. We performed experiments in temperature-controlled cultures to model the impact of \u003cem\u003ein vivo\u003c/em\u003e inflammation-associated heat, hypothesizing that immune-complex activated innate immune cells may generate heat, as suggested by our in vitro data. To begin to explore this, we stimulated pre-vaccination PBMC with the QIV at 37\u0026deg;C and 39\u0026deg;C for five days and monitored \u003cem\u003ein vitro\u003c/em\u003e B cell proliferation and differentiation into CD27\u003csup\u003ehigh\u003c/sup\u003eCD38\u003csup\u003ehigh\u003c/sup\u003e plasmablasts (PB). The detailed B cell gating strategy is shown in \u003cb\u003eSupplementary Fig.\u0026nbsp;1\u003c/b\u003e. QIV-stimulated B cells cultured at 39\u0026deg;C exhibited four-fold higher PB frequencies (36.5% vs. 9.6%, p\u0026thinsp;=\u0026thinsp;0.0039; Fig.\u0026nbsp;\u003cspan refid=\"Fig4\" class=\"InternalRef\"\u003e4\u003c/span\u003eA) and more than two-fold increased proliferation (50.2% vs. 20.5%, p\u0026thinsp;=\u0026thinsp;0.0039; Fig.\u0026nbsp;\u003cspan refid=\"Fig4\" class=\"InternalRef\"\u003e4\u003c/span\u003eB) compared to cells cultured at 37\u0026deg;C. Notably, we did not observe any effect of culture temperature when using non-BCR-mediated B cell stimulation with CD40L/IL-21 (Fig.\u0026nbsp;\u003cspan refid=\"Fig4\" class=\"InternalRef\"\u003e4\u003c/span\u003eA,B). Activating B cells with QIV at elevated temperatures enhanced polyclonal IgG production (Fig.\u0026nbsp;\u003cspan refid=\"Fig4\" class=\"InternalRef\"\u003e4\u003c/span\u003eC), resulted in a mild increase in IgM (\u003cb\u003eSupplementary Fig.\u0026nbsp;12\u003c/b\u003e), and was associated with a significant increase in influenza strain-specific IgG (Fig.\u0026nbsp;\u003cspan refid=\"Fig4\" class=\"InternalRef\"\u003e4\u003c/span\u003eD). However, HA-specific antibodies produced at 39\u0026deg;C had a lower avidity index in urea challenge assays than those produced at 37\u0026deg;C (0.81 vs 0.34, p\u0026thinsp;=\u0026thinsp;0.0039, Fig.\u0026nbsp;\u003cspan refid=\"Fig4\" class=\"InternalRef\"\u003e4\u003c/span\u003eE).\u003c/p\u003e \u003cp\u003e \u003c/p\u003e \u003cp\u003eThese findings suggest that an elevated temperature in the microenvironment of B cells promotes antigen-induced B cell activation, proliferation, and antibody secretion.\u003c/p\u003e \u003cp\u003e \u003cb\u003eA strong thermal reactogenicity associated with a high magnitude but low-avidity and poorly hemagglutinin inhibiting IgG response in vivo\u003c/b\u003e \u003c/p\u003e \u003cp\u003eThe thermal reaction at the vaccination site transiently exposes immune cells to elevated temperatures. Given the \u003cem\u003ein vitro\u003c/em\u003e evidence that heat modulates B cell activity, we next examined whether vaccine-induced immune responses differed between individuals with high (ΔT\u003csup\u003ehi\u003c/sup\u003e) and low (ΔT\u003csup\u003elo\u003c/sup\u003e) thermal reactivity. We assessed the frequencies of plasmablasts and T follicular helper (Tfh)-like T cells in the peripheral blood on day 7, along with T cell responses, antibody levels, HAI titers, and antibody avidity on day 28. An unsupervised hierarchical clustering analysis revealed that thermal reactogenicity, pre-vaccination HA-specific IgG1, and immune complex formation were strongly interconnected and associated with features of an extrafollicular B cell response (Fig.\u0026nbsp;\u003cspan refid=\"Fig5\" class=\"InternalRef\"\u003e5\u003c/span\u003eA).\u003c/p\u003e \u003cp\u003e \u003c/p\u003e \u003cp\u003eSubsequently, we performed direct group comparisons between the ΔT\u003csup\u003ehi\u003c/sup\u003e and ΔT\u003csup\u003elo\u003c/sup\u003e groups. Plasmablast egress from lymph nodes and the expansion of circulating Tfh-like T cells are hallmarks of the early influenza vaccine response in humans \u003csup\u003e\u003cspan citationid=\"CR34\" class=\"CitationRef\"\u003e34\u003c/span\u003e,\u003cspan citationid=\"CR35\" class=\"CitationRef\"\u003e35\u003c/span\u003e\u003c/sup\u003e. At baseline and on day 7, Tfh-like cell frequencies were comparable across groups (Fig.\u0026nbsp;\u003cspan refid=\"Fig5\" class=\"InternalRef\"\u003e5\u003c/span\u003eB). In contrast, ΔT\u003csup\u003ehi\u003c/sup\u003e subjects exhibited significantly higher frequencies of circulating plasmablasts at 7 days post-vaccination (Fig.\u0026nbsp;\u003cspan refid=\"Fig5\" class=\"InternalRef\"\u003e5\u003c/span\u003eC) and a more significant fold change compared to baseline (median: ΔT\u003csup\u003elo\u003c/sup\u003e 9.250 vs. ΔT\u003csup\u003ehi\u003c/sup\u003e 15.96 fold change, p\u0026thinsp;=\u0026thinsp;0.013). T cell intrinsic HA-specific IFNγ production at day 28 post-vaccination was non-significantly elevated in ΔT\u003csup\u003ehi\u003c/sup\u003e subjects (H1\u0026thinsp;+\u0026thinsp;H3 408 vs 544 SFC/M, p\u0026thinsp;=\u0026thinsp;0.3; QIV 510 vs. 629 SFC/M, p\u0026thinsp;=\u0026thinsp;0.2) (Fig.\u0026nbsp;\u003cspan refid=\"Fig5\" class=\"InternalRef\"\u003e5\u003c/span\u003eD). On average, the total hemagglutinin-specific IgG, specifically IgG1, against the vaccine strains at 28 days post-vaccination was 4-fold higher in subjects that exhibited strong thermal reactions (range 3.67\u0026ndash;4.22-fold higher in ΔT\u003csup\u003ehi\u003c/sup\u003e subjects) and correlated with the absolute temperature increase at the vaccination site (Fig.\u0026nbsp;\u003cspan refid=\"Fig5\" class=\"InternalRef\"\u003e5\u003c/span\u003eE, \u003cb\u003eSupplementary Fig.\u0026nbsp;13)\u003c/b\u003e. In contrast, post-vaccination sera from subjects with mild thermal reactogenicity demonstrated greater hemagglutinin inhibition titers (as a surrogate for virus neutralization capacity) against the H1 and H3 vaccine strains (Fig.\u0026nbsp;\u003cspan refid=\"Fig5\" class=\"InternalRef\"\u003e5\u003c/span\u003eF). Divergence in antigen-binding and neutralization capacity may be due to differentially targeted epitopes or to differences in antibody avidity. We found that vaccination-induced influenza-specific IgGs in ΔT\u003csup\u003ehi\u003c/sup\u003e subjects were of lower avidity than in those with mild thermal reactogenicity, as assessed by biolayer interferometry and urea challenge (Fig.\u0026nbsp;\u003cspan refid=\"Fig5\" class=\"InternalRef\"\u003e5\u003c/span\u003eG, \u003cb\u003eSupplementary Fig.\u0026nbsp;13\u003c/b\u003e). The QIV induced HA-specific IgG of all subclasses, but subclass distributions varied by HA specificity and thermal response profile, with IgG1 dominance in ΔT\u003csup\u003ehi\u003c/sup\u003e sera (\u003cb\u003eSupplementary Fig.\u0026nbsp;13\u003c/b\u003e). We then tested the d28 post-immunization serum for HA-IgG-IC-mediated THP-1 activation. HA-IgG-IC formed with post-vaccination (day 28) sera robustly activated THP-1 and enhanced ADCP, particularly when derived from ΔT\u003csup\u003ehi\u003c/sup\u003e individuals (Fig.\u0026nbsp;\u003cspan refid=\"Fig5\" class=\"InternalRef\"\u003e5\u003c/span\u003eH). All key findings were confirmed in complementary analyses using ΔT and the vaccine response readouts as continuous variables (\u003cb\u003eSupplementary Fig.\u0026nbsp;14\u003c/b\u003e).\u003c/p\u003e \u003cp\u003eThese data collectively link increased thermal reactogenicity to elevated pre-existing, non-neutralizing (i.e., low HAI titers) anti-HA antibodies that promote the formation of IgG1-enriched immune complexes. This Fcγ receptor- and/or complement-mediated activation was associated with higher antibody magnitude post-vaccination. These antibodies had lower avidity and exerted lower hemagglutinin inhibition, suggesting that local heat and immunecomplex-driven inflammation shape the qualitative outcome of the vaccine response.\u003c/p\u003e"},{"header":"Discussion","content":"\u003cp\u003eLocal reactogenicity is the most common adverse event following immunization, yet its immunological basis and consequences remain incompletely defined. In healthy adults receiving the seasonal influenza vaccine, we quantified the local temperature increase at the injection site and leveraged its broad inter-individual variability to dissect potential mechanisms underlying this response and its impact on adaptive immunity. Specifically, influenza vaccination triggered a measurable thermal reaction at 24 hours, enabling classification into high (ΔT\u003csup\u003ehi\u003c/sup\u003e) and low (ΔT\u003csup\u003elo\u003c/sup\u003e) responders.\u003c/p\u003e \u003cp\u003eWe found that immune complexes formed between HA-specific IgG and recombinant hemagglutinin bound and activated complement \u003cem\u003ein vitro\u003c/em\u003e. Similarly, HA-IgG-IC activated innate cells by engaging FcγR, thereby prompting monocyte activation, upregulating activation markers (HLA-DR and CD86), secreting inflammatory cytokines, and enhancing ADCP. The ΔThi subjects showed significantly higher levels of HA-specific IgG1 before vaccination. Additionally, the immune complexes with their serum exhibited significantly stronger FcγR-dependent immune activation and phagocytosis in monocytes. This underscores the role of pre-existing non-neutralizing IgG in promoting local inflammatory responses. These results diverge from a recent report that associated low baseline immunity with increased reactogenicity, although the lack of temperature measurements in that study limits direct comparison\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e21\u003c/span\u003e\u003c/sup\u003e. Moreover, we cannot exclude that other pathogen-specific IgG subclasses are more relevant than IgG1 in other vaccines or other clinical contexts.\u003c/p\u003e \u003cp\u003eConceptually, the pre-existing IgG against HA, forming HA-IgG-IC following immunization with HA and causing immune activation, represents a type III hypersensitivity (Arthus-like) reaction\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e19\u003c/span\u003e\u003c/sup\u003e. Unlike classical type III hypersensitivity, observed after exposure to an intravenous antigen that allows ICs to distribute to joints or other organs, the vaccine reaction is limited locally. Notably, the local thermal reaction, the baseline HA-specific IgG1, the HA-IgG-IC and FcR-mediated monocyte activation and ADCP were closely interlinked, and the amount of HA-IgG-IC correlated with the same baseline and outcome parameters as the ΔT (\u003cb\u003eFigure S9 and\u003c/b\u003e Fig.\u0026nbsp;\u003cspan class=\"InternalRef\"\u003e5\u003c/span\u003eA). Therefore, our study design prevents us from isolating the effects of immune complex-mediated complement activation and FcR-mediated monocyte activation on local heat production and reactogenicity. However, our data suggest that the overall innate activation is reflected clinically in the local thermal response, which serves as an easy, measurable, quantitative surrogate.\u003c/p\u003e \u003cp\u003eThe second key finding was that the local thermal reactivity was associated with downstream adaptive responses. Exploratory experiments using elevated culture temperatures \u003cem\u003ein vitro\u003c/em\u003e showed enhanced B cell proliferation, plasmablast differentiation, and antibody secretion, in line with emerging evidence that heat affects immune cell dynamics and trafficking\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e30\u003c/span\u003e\u003c/sup\u003e. These \u003cem\u003ein vitro\u003c/em\u003e experiments, however, were only an approximation of the \u003cem\u003ein vivo\u003c/em\u003e situation and did not investigate other plausible mechanisms by which temperature could affect adaptive immunity, such as accelerated antigen uptake and processing. \u003cem\u003eIn vivo\u003c/em\u003e, ΔT\u003csup\u003ehi\u003c/sup\u003e individuals mounted higher HA-specific total IgG and IgG1 responses by day 28, however, these antibodies exhibited reduced avidity in biolayer interferometry and urea-challenge assays and exhibited weaker hemagglutinin inhibition capacity (as a surrogate for neutralization). Collectively, this data suggests that heightened local inflammation may increase antibody quantity at the expense of avidity.\u003c/p\u003e \u003cp\u003ePrevious studies have reported higher local reactogenicity and immunogenicity in women; however, most examined mRNA or adjuvanted vaccines and did not quantify local thermal responses, limiting direct comparison\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e36\u003c/span\u003e\u003c/sup\u003e. Fever after influenza vaccination has been associated with higher hemagglutination inhibition titers\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e37\u003c/span\u003e\u003c/sup\u003e, however, no participants in our study developed fever. Gromer at al. reported that local reactions were associated with lower pre-existing IgG levels, although local thermal responses were not assessed\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e21\u003c/span\u003e\u003c/sup\u003e.\u003c/p\u003e \u003cp\u003eThe inactivated influenza vaccine has an excellent safety profile, but local reactogenicity is common (30–50% of vaccinated subjects)\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e38\u003c/span\u003e\u003c/sup\u003e. Traditional studies investigating associations between reactogenicity and immunogenicity have relied on easily accessible measures such as pain, swelling, or fever. However, these are subjective, difficult to quantify, or may depend on the vaccine administration technique\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e39\u003c/span\u003e\u003c/sup\u003e. Temperature measurement provides an attractive, objective, and quantifiable alternative. Prior work using infrared imaging similarly reported heterogeneous thermal responses, yet without evaluating their immunological consequences \u003csup\u003e\u003cspan class=\"CitationRef\"\u003e40\u003c/span\u003e\u003c/sup\u003e. They reported a mean temperature increase of + 0.70°C at 24h post-vaccination, with 40% experiencing a thermal reaction of at least + 1°C. Our \u003cem\u003ein vitro\u003c/em\u003e data further suggest that immune cells themselves may contribute to local heat production, potentially via mitochondrial uncoupling. Mitochondria physiologically maintain temperatures that exceed core body temperature, which may reach 50°C in activated mitochondria \u003csup\u003e\u003cspan class=\"CitationRef\"\u003e41\u003c/span\u003e\u003c/sup\u003e. The relevance of these mechanisms to vaccine reactogenicity remains to be further defined.\u003c/p\u003e \u003cp\u003eThe observation that pre-existing immunity shapes the adaptive vaccine response is not novel. The concept of antibody feedback summarizes the interference of pre-existing antigen-specific antibodies with the subsequent evolution of adaptive immunity upon revaccination or reinfection\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e6\u003c/span\u003e\u003c/sup\u003e. Thereby, immune complexes can enhance antigen uptake and presentation, potentially resulting in a more efficient antigen presentation and a more robust adaptive immune response \u003csup\u003e\u003cspan class=\"CitationRef\"\u003e42\u003c/span\u003e\u003c/sup\u003e. However, antigen uptake in macrophages may limit antigen availability for B cell activation and sustained germinal center engagement. Similarly, pre-existing antibodies may mask epitopes, potentially promoting high-affinity B cell responses \u003csup\u003e\u003cspan class=\"CitationRef\"\u003e43\u003c/span\u003e\u003c/sup\u003e, select for B cell responses against subdominant or less conserved epitopes (32), or prevent antigen uptake or B cell stimulation through interference \u003csup\u003e\u003cspan class=\"CitationRef\"\u003e13\u003c/span\u003e,\u003cspan class=\"CitationRef\"\u003e44\u003c/span\u003e,\u003cspan class=\"CitationRef\"\u003e45\u003c/span\u003e\u003c/sup\u003e. However, our data do not support this hypothesis, as increased IC uptake was associated with an extrafollicular response phenotype with low-avidity antibodies on day 28.\u003c/p\u003e \u003cp\u003eThe HA-IgG-IC associated enhanced FcR-mediated innate activation, including monocyte activation, shapes the inflammatory milieu at the vaccination site. Strong innate inflammation associated with a features of a extrafollicular B cell response in our clinical cohort. Specifically, we observed a pronounced early plasmablast response at day 7 post-immunization and lower-avidity HA-specific IgG at day 28, in relation to strong thermal reactions. In this context, elevated local temperature may act as a modulatory factor rather than a primary driver, potentially influencing cellular metabolism, activation kinetics, or antigen processing during early immune response events. As a complementary explanation, accelerated extrafollicular responses may be fueled by preferential activation of memory B cells primed from prior influenza exposures, potentially further limiting the amount of antigen available for prolonged germinal center reactions and de novo affinity maturation. Future research should evaluate the baseline level of HA-specific memory B cells to explore their role in competing for and scavenging antigens. Including BCR sequencing data will help determine whether germinal center reactions are altered in individuals with strong local thermal reactions. Finally, vaccine antigen-IgG immunocomplexes increase the size and valency of the vaccine antigen. High-valency antigens induce a low-affinity, extrafollicular response, whereas smaller, low-valency antigens activate the high-affinity B cells preferentially\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e46\u003c/span\u003e\u003c/sup\u003e. Collectively, these mechanisms may explain the observed phenotype of extrafollicular B cell responses in those with a strong local temperature reaction and strong IC activation.\u003c/p\u003e \u003cp\u003eStudies with IC-based vaccine strategies and Fc-engineered HA-Fc constructs have demonstrated that antibody glycosylation and Fc configuration can profoundly influence B cell selection, raising the possibility that qualitative features of pre-existing antibodies, not only their abundance, modulate vaccine outcomes. HA-IgG-IC have been explored as potential vaccine constructs in preclinical models and in humans \u003csup\u003e\u003cspan class=\"CitationRef\"\u003e47\u003c/span\u003e–\u003cspan class=\"CitationRef\"\u003e49\u003c/span\u003e\u003c/sup\u003e. \u003cem\u003eIn vivo\u003c/em\u003e, human influenza vaccine efficacy correlated with the amount of sialylated Fc on anti-HA-IgG produced during the early plasmablast response. The authors demonstrated that this improved humoral vaccine response occurs through co-engagement of the sialylated Fc region with CD23, which triggers the inhibitory FcγRIIB. This process raises the antigenic threshold and favors the selection of high-affinity B cells cells\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e50\u003c/span\u003e\u003c/sup\u003e. In preclinical studies, ICs consisting of the influenza vaccine and sialylated Fc anti-HA-IgG were used to immunize mice. IC vaccination elicited higher-avidity antibody responses than HA alone, with qualitatively enhanced breadth and potency against influenza viruses\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e51\u003c/span\u003e\u003c/sup\u003e. A modified approach to harnessing IC in influenza vaccination is fusing HA to an Fc fragment. Immunization with these fusion proteins induced broad immune responses and high cross-clade protection in mice\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e52\u003c/span\u003e\u003c/sup\u003e. Combined, this suggests that not only the amount of pre-existing IgG, but also the glycosylation of the Fc part, which critically informs the effector function of the IgGs, are important to consider.\u003c/p\u003e \u003cp\u003eOur study's strengths include the integration of \u003cem\u003ein vivo\u003c/em\u003e and \u003cem\u003ein vitro\u003c/em\u003e systems and the detailed temporal profiling, which allows us to unravel associations between immune features and the reactogenicity phenotype. We investigated immune complex-mediated immune activation in mechanistic detail and demonstrate that immune cells may produce heat \u003cem\u003ein vitro\u003c/em\u003e in a multi-modal approach. Limitations include the sample size, absence of a validation cohort, and female predominance in the ΔT\u003csup\u003ehi\u003c/sup\u003e subjects. We, therefore, cannot exclude that sex, hormonal differences, or relatively higher vaccine doses (per body mass compared to men) contributed to the observed phenotype. Notably, many immune genes are located on the X chromosome, including the innate sensor TLR7\u003csup\u003e53\u003c/sup\u003e and the literature consistently reports higher local reactogenicity and immunogenicity to the inactivated influenza vaccine in females (reviewed in\u003csup\u003e54\u003c/sup\u003e). In contrast, systemic reactions occur with similar frequencies. Sex-related differences in hormones, skin thickness, blood flow, and the nervous system's structure may promote the development of injection-site inflammation in females \u003csup\u003e\u003cspan class=\"CitationRef\"\u003e54\u003c/span\u003e\u003c/sup\u003e.\u003c/p\u003e \u003cp\u003eExperimental limitations include that we only assessed immune complex formation and activation indirectly \u003cem\u003ein vitro\u003c/em\u003e, as we did not perform muscle biopsies. Similarly, since direct assessment of neutrophil recruitment requires tissue sampling or whole-blood analysis, we focused on monocytes as an innate cell subset. Histopathological studies on local vaccine reactogenicity have been done mostly for specific vaccines. In humans, a combined PET/CT and needle biopsy study for transcriptomics investigated gene signatures following intramuscular immunization with an adjuvanted, but not the standard, influenza vaccine\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e55\u003c/span\u003e\u003c/sup\u003e. Mouse studies compared histopathologic findings one month post-immunization with various vaccines, including the influenza vaccine. The timing of sampling and the absence of pre-existing immunity in this animal study preclude conclusions regarding immune complex formation\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e56\u003c/span\u003e\u003c/sup\u003e. Whether it is appropriate to perform muscle biopsies in human volunteers following a seasonal influenza vaccine for research purposes is debatable. Animal models with pre-existing pathogen-specific immunity could be employed to study local immune complex formation and complement activation in the future.\u003c/p\u003e \u003cp\u003eFinally, we cannot exclude that affinity maturation in subjects with strong local reactogenicity follows a different trajectory that was missed due to the single later timepoint at 28 days post immunization. Studies in humans have shown that following repeated immunization with the flu vaccine, affinity maturation is limited and often completed within four weeks\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e57\u003c/span\u003e,\u003cspan class=\"CitationRef\"\u003e58\u003c/span\u003e\u003c/sup\u003e but can extend over months\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e59\u003c/span\u003e\u003c/sup\u003e.\u003c/p\u003e \u003cp\u003eIn conclusion, our study provides novel insights into the relationship between vaccine reactogenicity and pre-existing humoral immunity in standard, non-adjuvanted influenza protein vaccination. The findings underscore the importance of considering both the magnitude and quality of the immune response when evaluating the consequences of vaccine-induced reactogenicity. Further research is necessary to determine whether adjusting the thermal response at the injection site or via metabolic interventions can improve vaccine efficacy by balancing reactogenicity and immunogenicity. Conducting a clinical study to assess if non-steroidal anti-inflammatory drugs (NSAIDs) influence local thermal reactogenicity and subsequent immune responses would be relatively simple. Interestingly, in pediatric studies, NSAIDs did not significantly affect antibody responses to various vaccines vaccines\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e60\u003c/span\u003e,\u003cspan class=\"CitationRef\"\u003e61\u003c/span\u003e\u003c/sup\u003e, although none of these studies tested antibody avidity or HAI titers as functional outcomes. Understanding how local inflammation and IC-driven pathways modulate vaccine immunogenicity may inform strategies to optimize antigen design, Fc engineering, and formulation to enhance protective immunity while limiting unwanted reactogenicity.\u003c/p\u003e "},{"header":"Methods","content":"\u003ch2\u003eStudy participants\u003c/h2\u003e\u003cp\u003e The local ethics committee (Ethics Commission of North-Western and Central Switzerland, EKNZ #2017 − 01726) approved the study (ARIVA-Study; NCT04059991, registration date on ClinicalTrials.gov: 2017-11-01) that was conducted in accordance with the Declaration of Helsinki. All subjects were healthy, provided written informed consent, and received no other vaccinations during the study. None of the study participants reported use of non-steroidal anti-inflammatory drugs (NSAIDs) during the 24 hours after the vaccination, or was taking corticosteroids, biologics, or other immunomodulatory medications. The majority of participants were healthcare workers or laboratory personnel. All subjects were vaccinated between November and December 2019 with the same inactivated, non-adjuvanted, quadrivalent influenza split vaccine (Vaxigrip Tetra, Sanofi 2019/20), containing 15 µg hemagglutinin per strain (A/Brisbane/02/2018; A/Kansas/14/2017; B/Colorado/06/2017; and B/Phuket/3073/2013) in a total volume of 0.5 mL. We gathered data through a questionnaire on self-reported influenza-like illness over the last five years, the total number of influenza vaccines received during this period, personal histories of allergic diseases and autoimmunity, and demographic details including sex, BMI, and age.\u003c/p\u003e\u003cp\u003e \u003cem\u003eAssessment of reactogenicity and local thermal reactions.\u003c/em\u003e \u003c/p\u003e\u003cp\u003eWe utilized a contact-free temporal thermometer (Withings, Europe) for all temperature assessments. According to the company, this thermometer employs 16 infrared sensors to take over 4,000 measurements within seconds (HotSpot Sensor Technology). It operates within a range of 35°C to 43.2°C (95°F to 109.8°F), featuring a resolution of 0.1°C (0.2°F and a clinical accuracy of ± 0.2°C (± 0.4°F) for measurements in the temporal area. We measured the temperature at the vaccine injection site (deltoid region) immediately before and 24 hours after vaccination, as well as at the same location on the opposite arm and both temporal regions (i.e., systemic temperature) for comparison. Measurements were conducted in duplicate, and average values were calculated to determine the temperature difference before and after vaccination at the injection site [ΔT (24h-0h)], between the vaccinated and control arm [ΔT(vaccine)-(control)], or systemically. The ‘local thermal response’ was defined as the ΔT at the vaccination arm. In addition, study participants subjectively rated their pain 24 hours post-vaccination as: none, mild, or strong. We examined the vaccination site for erythema (redness) and, if present, measured the largest diameter in centimeters (cm).\u003c/p\u003e\u003ch3\u003eSampling and peripheral blood mononuclear cell (PBMC) isolation\u003c/h3\u003e\u003cp\u003eWe collected serum and ethylenediaminetetraacetic acid (EDTA) blood samples before, after 24 hours, and on days 7 and 28 post-vaccination for immunological analyses. To isolate the PBMC fraction, the EDTA blood was diluted in PBS and layered over 16.5 ml Lymphoprep medium (density 1.077 g/ml) in centrifuge Leucosep tubes (Grainer Bio-One, Austria). PBMCs were isolated by standard Ficoll-Paque density-gradient centrifugation at 700×g for 15 minutes with a low acceleration and no breaks\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e62\u003c/span\u003e\u003c/sup\u003e. The enriched PBMC layer was collected and washed twice in PBS, and cells were used immediately or cryopreserved in FBS containing 10% DMSO until further use.\u003c/p\u003e\u003ch2\u003eElispot to measure influenza-specific T cell responses\u003c/h2\u003e\u003cp\u003eStandard IFN-γ Elispot was performed using 150,000 PBMC/well. We stimulated the cells with 1µg/ml recombinant hemagglutinin (A/Brisbane/02/2018 (H1N1) and A/Kansas/14/2017 (H3N2)) (both from (eENZYME LLC, Gaithersburg, MD, USA) or with the commercial influenza vaccine (QIV; Vaxigrip Tetra, Sanofi 2019/20) in a 1:200 dilution on a IFNγ-coated PVDF (polyvinylidene fluoride) plate (Mabtech, Nacka Strand, Sweden) at 37°C, 5% CO\u003csub\u003e2\u003c/sub\u003e for 18 hours. 0.5 µg/mL SEB (staphylococcal enterotoxin B) for polyclonal T cell activation or media alone served as controls. Elispot data were expressed as spot-forming cells per million PBMC (SFU/M).\u003c/p\u003e\u003ch2\u003eMeasurement of the influenza-specific antibodies by multiplexed Luminex assay\u003c/h2\u003e\u003cp\u003eUsing a custom-made Luminex assay, we quantified antibodies specific to the H1 and H3 vaccine strain. Different Luminex MaxPlex®beads were coated with recombinant hemagglutinin (HA) from the vaccine strains A/Brisbane/02/2018 (H1N1) and A/Kansas/14/2017 (H3N2) according to the manufacturer’s instructions. Briefly, 1.25µg of HA protein was coupled onto 1.25\u0026nbsp;million beads in 500µl of 50 mM MES buffer (pH 5.0) for 2h at RT with constant rotation. The bead coupling to different HA was verified using an anti-His antibody (1 µg/mL, A00174, GenScript) and a PE-labeled anti-rabbit IgG secondary antibody (1 µg/mL, 406421, BioLegend) that detects the his-tag on the HA. To measure HA-specific serum IgG, we incubated 1000 beads with sera diluted 1:100 and following the manufacturer’s instructions\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e63\u003c/span\u003e\u003c/sup\u003e. We used 1 µg/mL of the respective mouse anti-human detection antibodies to quantify Influenza-specific IgM (SA-DA4), IgG (JDC-10), IgG1-4 subclasses (HP6001, HP6002, HP6050, HP6025) and IgA (2053-01; all from SouthernBiotech, Birmingham, AL, USA). Bovine serum albumin (BSA)-coated beads were the negative control. Data was acquired as median fluorescence intensity (MFI) on a Luminex 200 reader. To compare subclass-specific responses between groups, we calculated relative responses per immunoglobulin class and antigen, i.e. median MFI ΔT\u003csup\u003ehi\u003c/sup\u003e divided by MFI ΔT\u003csup\u003elo\u003c/sup\u003e.\u003c/p\u003e\u003ch2\u003eHemagglutination inhibition assay\u003c/h2\u003e\u003cp\u003eWe measured influenza strain-specific hemagglutination inhibition (HAI) titers against A/Brisbane/02/2018 (H1N1) and A/Kansas/14/2017 (H3N2) (NIBSC, Hertfordshire, UK)\u003csup\u003e\u003cspan class=\"CitationRef\"\u003e64\u003c/span\u003e\u003c/sup\u003e. The influenza virus concentration was adjusted to four hemagglutination units (HAU) in a standard hemagglutination assay. Pre- and post-vaccination sera were treated with a receptor-destroying enzyme (Denka Seiken Co., Ltd, Tokyo, Japan) for 18 hours at 37°C, followed by heat-inactivation at 56°C for one hour. Samples were diluted two-fold serially in PBS in duplicates and mixed 1:1 with the virus. After one hour at 37°C, formaldehyde-fixed guinea pig red blood cells (1.5%) were added and incubated for one hour at 4°C\u003csup\u003e64\u003c/sup\u003e. The HAI titer was defined as the highest serum dilution that inhibited hemagglutination.\u003c/p\u003e\u003ch2\u003eHemagglutinin-IgG immune complex formation, C1q binding assay and in vitro complement activation\u003c/h2\u003e\u003cp\u003eHemagglutinin-IgG immune complexes (HA-IgG-IC) were generated by mixing the recombinant HA at 0.5µg/mL HA (HA used as described above) with participants’ sera at a 1:10 dilution. Complement binding capacity of the HA-IgG-IC was assessed using the QUANTA Lite C1q CIC ELISA (Inova Diagnostics/Werfen, Barcelona, Spain) following the manufacturer’s instructions. Briefly, HA-IgG-IC were incubated in C1q-coated microplate wells, and C1q binding of the IC was detected using a horseradish peroxidase–conjugated goat anti-human IgG antibody and quantified by measuring absorbance at 450nm. Immune complex concentrations were extrapolated from the calibration curve and expressed as heat-aggregated human IgG equivalents per mL (µg Eq/mL).\u003c/p\u003e\u003cp\u003eTo assess in vitro complement activation, we coated plates with 5 µg/mL C1q protein (Complement Technology Inc., Tyler, TX, USA) in 0.2 M carbonate buffer (pH 9.6) overnight at 4°C., blocked with PBS + 1% BSA. Serum samples were diluted 1:50 in either HBS (HEPES-buffered saline) or PBS supplemented with 10 mM EDTA and incubated on the plates for 1 h at 37°C with shaking at 300 rpm. Complement activation was assessed by detecting C4d deposition using rabbit anti-human C4d (Abcam, Cambridge, UK, 1:400) followed by HRP-conjugated donkey anti-rabbit IgG (BioLegend, San Diego, CA, USA, 1:4000) and TMB substrate (Invitrogen, Waltham, MA, USA), and absorbance was measured at 450 nm\u003csup\u003e28\u003c/sup\u003e.\u003c/p\u003e\u003ch2\u003eAntibody avidity determination using Biolayer Interferometry (BLI) and urea challenge\u003c/h2\u003e\u003cp\u003eTo assess anti-HA-antibody avidity by biolayer interferometry, 10 µg/mL His-tagged hemagglutinin (A/Brisbane/02/2018 (H1N1) and A/Kansas/14/2017 (H3N2)) was loaded onto Ni-NTA biosensors (Sartorius, Göttingen, Germany) in running buffer (PBS, 0.02% Tween-20, 0.1% BSA) for 300 s. Sensors were dipped in running buffer for 60 s, then into serum-containing buffer for association (300 s), followed by dissociation in buffer for 600 s. Regeneration involved three cycles of 20 mM glycine in PBS, alternating with running buffer, followed by reactivation in 20 mM NiCl₂ for 120 s. All steps were performed at 1000 rpm. KD values were calculated using Octet® CFR software (ForteBio, Fremont, CA, USA). In select experiments, IgG avidity was assessed in addition (or solely) by urea challenge, comparing Luminex MFI values of HA-specific IgG after 30 min incubation with either PBS or 6 M urea (room temperature, 800 rpm). The avidity index (AI) was defined as [MFI with incubation in urea solution] / [MFI with incubation in PBS].\u003c/p\u003e\u003ch2\u003eMonocyte phenotyping, in vitro maturation and antibody-dependent cellular phagocytosis assay\u003c/h2\u003e\u003cp\u003ePrimary monocytes were isolated from PBMC taken at the pre-vaccination timepoint from subjects with low and high local temperature reactions. Monocyte subsets were sorted on a FACSAria® III (BD Biosciences) using CD3 (Alexa Fluor 700, OKT3), CD19 (Alexa Fluor 488, HIB19), CD14 (FITC, 63D3), CD16 (BUV 496, 3G8), and a viability dye (eFluorTM 780, Invitrogen™). Sorted monocytes or the monocyte cell line THP-1 (ATCC® TIB-202™) were differentiated into monocyte-derived dendritic (mDC) cells for five days in the presence of 1000 U/ml GM-CSF and IL-4 each, replenished at days 2 and 4. For mDC maturation, 200 pg/ml LPS was added for 24 hours. \u003cem\u003eEx vivo\u003c/em\u003e monocytes and mDCs were incubated with fluorochrome-coupled hemagglutinin in the presence or absence of sera (1:10) from subjects with low- or high-temperature reactions, for four hours. Fluorochrome-coupling of the H3N2 A/Kansas/14/2017 hemagglutinin (10 µg/reaction) was performed using the Lightning-Link® Allophycocyanin (APC) conjugation kit (Expedeon, San Diego, CA, USA) according to the manufacturer’s instructions. Briefly, 10ug hemagglutinin was mixed with the Modifier reagent at a ratio of 1:10. The antibody-Modifier mixture was added directly to a vial containing lyophilized fluorochrome conjugation mix (APC) and resuspended by gentle pipetting. The reaction was incubated for 3 h at room temperature in the dark. Following incubation, Quencher reagent was added at a 1:10 ratio, gently mixed and incubated for 30 min at room temperature. The resulting conjugated antibody was ready for use without further purification. Activation and HA uptake were assessed by flow cytometry. Antibodies used to characterize the monocyte activation profile are listed in \u003cb\u003eSupplementary Table\u0026nbsp;1.\u003c/b\u003e A viability dye (eFluorTM 780, Invitrogen™) was included in all experiments.\u003c/p\u003e\u003cp\u003eIn vitro cytokine production was quantified in the culture supernatants of monocytes activated as indicated in the respective experiments. We used ELISA kits for IL-1 and IL-6 (Peprotech, Cranbury, NJ, USA) according to the manufacturer’s instructions. For the Fc-receptor blocking experiments, we used antibodies against FcγR1 (CD64, 10.1) [10 µg/ml]), FcγR2 (CD32, FUN-2) [10 µg/ml]), and FcγR3 (CD16, 3GB) [10 µg/ml]) (all from BioLegend). THP-1 monocytes were preincubated with blocking antibodies for one hour before adding fluorochrome-labeled hemagglutinin and serum. The effect of blocking was calculated as percent inhibition ((H3 uptake without blocking / H3 uptake with the Fc block)*100). After four hours of incubation, cells were stained using antibodies listed in \u003cb\u003eSupplementary Table\u0026nbsp;1\u003c/b\u003e and acquired on a BD LSRFortessa. Analysis was performed using FlowJo v.20.6.2.\u003c/p\u003e\u003ch2\u003eIn vitro temperature measurements of cellular heat production\u003c/h2\u003e\u003cp\u003eTHP-1, PBMCs, or sorted cell subsets were resuspended in complete RPMI medium and transferred into a DeepWell 96 U well plate. After an acclimatization period of 1 hour at 37°C, the cells were stimulated with HA-IgG-IC, LPS [1ng/ml, for monocyte activation], CpG [1 µg/ml, for B cell activation], anti-CD3/CD28 antibodies [2 µg/ml, for T cell activation], PMA [0.1 µg/ml, for NK cell activation] or maintained in the medium as a control. The temperature of the culture medium was recorded every minute during the acclimatization period and a three-hour stimulation using a data logger thermometer (SEFRAM9814 Datenlogger-Thermometer) with a liquid-compatible immersion probe (TC type K. Testo). The average temperature for the entire three-hour period was summarized in bar graphs.\u003c/p\u003e\u003ch2\u003eMitochondrial temperature production assay using MitoThermo Yellow (MTY)\u003c/h2\u003e\u003cp\u003eTHP-1 or human primary monocytes were stimulated with the quadrivalent influenza vaccine [1:200] or LPS [1ng/ml] for six hours at 37°C, 5% CO\u003csub\u003e2\u003c/sub\u003e. Cells were then stained with 100nM MTY, 100nM MitoTracker Green (Invitrogen, Waltham, MA, USA), or both for 20 minutes at 37°C and 5% CO\u003csub\u003e2\u003c/sub\u003e. After washing, the cells were fixed and permeabilized with the BD fixation and permeabilization solution, and counterstained with DAPI (Biolegend, San Diego, CA, USA). Cells were mounted with Vectashield fluorescence mounting medium (Vector Laboratories, Burlingame, CA, USA) and analyzed using the Nikon A1 confocal microscope with a 100x oil-immersion objective (Nikon Plan Apo 100x 1.45NA oil). Stacked images were acquired at 0.1 mm intervals throughout the cell body. The fluorescence intensity of MTY overlapping with MitoTracker staining was quantified using ImageJ (Fiji, v.2.9.0). Data are expressed as MFI.\u003c/p\u003e\u003ch2\u003eTemperature effects on B cell function in vitro\u003c/h2\u003e\u003cp\u003eTo study the direct effects of higher temperature on immune cells, specifically B cells, we performed experiments at different cell culture temperatures. To this end, we set the incubator temperature set-point to 37.5°C or 39°C. The 39°C was chosen to approximate the elevated tissue temperature at the vaccination site. The estimate was based on the observed increase in skin surface temperature. The readouts focused on B-cell functions. PBMCs from the pre-vaccination time point were stimulated with the influenza vaccine (Vaxigrip®) [1/200] or a combination of CD40L [100 ng/ml] and IL-21 [100 ng/ml] at 37°C or 39°C. To assess proliferation, PBMCs were stained with the CellTrace™ Violet Cell Proliferation Kit (Thermo Fisher Scientific, Waltham, Massachusetts, USA) according to the manufacturer’s instructions before stimulation. On day five, proliferation was quantified as %CTV low B cells among total B cells and plasmablast generation was assessed using antibodies listed in \u003cb\u003eSupplementary Table\u0026nbsp;1\u003c/b\u003e and a viability dye (eFluor™ 780, Invitrogen™). All flow cytometric experiments were acquired on an LSRFortessa (BD Biosciences, San Jose, CA) and analyzed using FlowJo (v.10.6.2). Total antibody production in the cultures was assessed after 7 days using an IgG and IgM ELISA (Invitrogen, Waltham, Massachusetts, USA). The influenza-specific IgG levels were measured using the multiplexed Luminex assay as described.\u003c/p\u003e\u003ch2\u003eDirect ex vivo immune cell phenotyping\u003c/h2\u003e\u003cp\u003ePeripheral blood mononuclear cells (PBMC) were stained immediately following isolation (as described above) for immuophenotyping. The antibodies used for \u003cem\u003ein vivo\u003c/em\u003e T cell, B cell, and Monocyte phenotyping are listed in \u003cb\u003eSupplementary Table\u0026nbsp;2\u003c/b\u003e. A viability dye (eFluor™ 780, Invitrogen™) was included in all panels. All samples were acquired on a BD LSRFortessa (BD Biosciences, San Jose, CA) and analyzed using FlowJo v.10.9.0. Gating strategies are indicated in the \u003cb\u003eSupplementary Figs.\u0026nbsp;1 and 2\u003c/b\u003e.\u003c/p\u003e\u003ch2\u003eData analysis and statistics\u003c/h2\u003e\u003cp\u003eGroup comparisons were performed using non-parametric, two-tailed t-tests (Mann-Whitney). We considered p-values \u0026lt; 0.05 statistically significant and reported the detailed p-values in the results and figure legends. Correlations of continuous variables were assessed using the non-parametric Spearman’s rank correlation. Comparisons of more than two groups were done using one-way ANOVA and Dunn’s test. Data was visualized using GraphPad Prism (Version 10.4.2).\u003c/p\u003e"},{"header":"Declarations","content":" \u003ch2\u003eCompeting Interest Statement\u003c/h2\u003e \u003cp\u003eThe Authors declare no competing financial or non-financial interest in relation to the study. C.T.B. is chair of the Swiss National Immunization Technical Advisory Group (NITAG).\u003c/p\u003e\u003ch2\u003eAuthor Contribution\u003c/h2\u003e\u003cp\u003eJ.R.H. performed experiments/generated data, analyzed and visualized the data, and drafted the manuscript. S.S. recruited and sampled subjects and coordinated the study. G.B. and M.R. provided support in designing the experiments and interpreting the data. C.T.B. designed the study, analyzed data, funded the study, and drafted the manuscript. All authors contributed to the writing of the manuscript.\u003c/p\u003e\u003ch2\u003eAcknowledgement\u003c/h2\u003e\u003cp\u003eThis work was supported by the Margot and Erich Goldschmidt \u0026amp; Peter Ren\u0026eacute; Jacobson-Stiftung and the Swiss National Science Foundation (SNSF; grant 310030_192440 to C.T.B.). We thank Vanessa Durandin (University Hospital Basel, Switzerland) for study nurse support of the clinical study, Prof. Philippe Kaiser and Dr. Ana Gonzalez (Geneva University Hospitals (HUG), Switzerland) for sharing their protocol for the hemagglutinin inhibition assays, Dr. Ingmar Heijnen (University Hospital Basel, Switzerland) for the input on measuring immunocomplexes, and Prof. Marten Trendelenburg (University Hospital Basel, Switzerland) for guidance on the in vitro complement activation assay. MitoThermo Yellow (MTY) was a kind gift from Prof. Y.T. Chang (Pohang University (POSTECH), Korea).\u003c/p\u003e\u003ch2\u003eData Availability\u003c/h2\u003e\u003cp\u003eAll data will be made available by the authors on reasonable request.\u003c/p\u003e"},{"header":"References","content":"\u003col\u003e\u003cli\u003e\u003cspan\u003ePollard, A. J. \u0026amp; Bijker, E. M. 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In this prospective human cohort receiving seasonal influenza vaccination, high baseline hemagglutinin-specific IgG1 levels were associated with more pronounced local thermal responses at the vaccinated arm and greater vaccine-induced antibody levels. These IgG antibodies formed immune complexes with hemagglutinin, activated complement and enhanced Fc-receptor-dependent monocyte activation and phagocytosis \u003cem\u003ein vitro\u003c/em\u003e, connecting pre-existing immunity to innate activation and local reactogenicity. Despite higher antibody levels and early plasmablast responses in subjects with strong thermal reactogenicity after vaccination, we observed lower avidity and hemagglutinin-inhibition capacity, suggesting extrafollicular responses. T cell responses were unaltered. These findings suggest an immune complex-mediated pathway through which pre-existing hemagglutinin-specific IgG amplify local thermal reactogenicity and modulate vaccine response quality, providing mechanistic insight into how prior immunity shapes human vaccine responsiveness.\u003c/p\u003e","manuscriptTitle":"Preexisting IgG forms immune complexes and links local thermal reactogenicity with immunogenicity in influenza vaccination","msid":"","msnumber":"","nonDraftVersions":[{"code":1,"date":"2026-03-31 17:43:26","doi":"10.21203/rs.3.rs-8338543/v1","editorialEvents":[{"type":"communityComments","content":0},{"type":"decision","content":"Revision requested","date":"2026-04-13T20:42:10+00:00","index":"","fulltext":""},{"type":"editorInvitedReview","content":"","date":"2026-04-12T21:51:41+00:00","index":"hide","fulltext":""},{"type":"editorInvitedReview","content":"","date":"2026-04-11T18:48:41+00:00","index":"hide","fulltext":""},{"type":"editorInvitedReview","content":"","date":"2026-04-06T15:50:16+00:00","index":"hide","fulltext":""},{"type":"editorInvitedReview","content":"","date":"2026-04-01T21:28:45+00:00","index":"hide","fulltext":""},{"type":"editorInvitedReview","content":"","date":"2026-03-30T05:53:19+00:00","index":"hide","fulltext":""},{"type":"reviewerAgreed","content":"323150671916533942512551553340477424429","date":"2026-03-29T18:56:35+00:00","index":"hide","fulltext":""},{"type":"reviewerAgreed","content":"60742724747583716519959793148372726982","date":"2026-03-29T03:54:32+00:00","index":"hide","fulltext":""},{"type":"reviewerAgreed","content":"232250208496018386419660538213210237920","date":"2026-03-28T13:43:51+00:00","index":"hide","fulltext":""},{"type":"reviewerAgreed","content":"296140127573572232133108900980864013597","date":"2026-03-27T14:14:23+00:00","index":"hide","fulltext":""},{"type":"reviewerAgreed","content":"93168623698817184875231679380509049914","date":"2026-03-26T23:34:00+00:00","index":"hide","fulltext":""},{"type":"reviewersInvited","content":"","date":"2026-03-26T13:39:35+00:00","index":"","fulltext":""},{"type":"checksComplete","content":"","date":"2026-03-26T09:58:10+00:00","index":"","fulltext":""},{"type":"submitted","content":"npj Vaccines","date":"2026-03-10T16:59:51+00:00","index":"","fulltext":""}],"status":"published","journal":{"display":true,"email":"[email protected]","identity":"npj-vaccines","isNatureJournal":false,"hasQc":true,"allowDirectSubmit":false,"externalIdentity":"npjvaccines","sideBox":"Learn more about [npj Vaccines](http://www.nature.com/npjvaccines/)","snPcode":"41541","submissionUrl":"https://submission.springernature.com/new-submission/41541/3?","title":"npj Vaccines","twitterHandle":"","acdcEnabled":true,"dfaEnabled":true,"editorialSystem":"stoa","reportingPortfolio":"NPJ","inReviewEnabled":true,"inReviewRevisionsEnabled":true}}],"origin":"","ownerIdentity":"6191fdf5-6562-4c75-9aeb-82ce0b12bd60","owner":[],"postedDate":"March 31st, 2026","published":true,"recentEditorialEvents":[],"rejectedJournal":[],"revision":"","amendment":"","status":"published-in-journal","subjectAreas":[{"id":65327514,"name":"Biological sciences/Immunology"},{"id":65327515,"name":"Biological sciences/Microbiology"}],"tags":[],"updatedAt":"2026-05-05T10:00:21+00:00","versionOfRecord":{"articleIdentity":"rs-8338543","link":"https://doi.org/10.1038/s41541-026-01477-x","journal":{"identity":"npj-vaccines","isVorOnly":false,"title":"npj Vaccines"},"publishedOn":"2026-05-02 15:58:33","publishedOnDateReadable":"May 2nd, 2026"},"versionCreatedAt":"2026-03-31 17:43:26","video":"","vorDoi":"10.1038/s41541-026-01477-x","vorDoiUrl":"https://doi.org/10.1038/s41541-026-01477-x","workflowStages":[]},"version":"v1","identity":"rs-8338543","journalConfig":"researchsquare"},"__N_SSP":true},"page":"/article/[identity]/[[...version]]","query":{"redirect":"/article/rs-8338543","identity":"rs-8338543","version":["v1"]},"buildId":"XKTyCvWXoU3ODBz1xrDgd","isFallback":false,"isExperimentalCompile":false,"dynamicIds":[84888],"gssp":true,"scriptLoader":[]}