Aging predisposes to acute inflammatory induced pathology after tumor immunotherapy

We have previously shown the IT regimen using an agonist anti-CD40 monoclonal antibody in combination with IL-2 to synergize and induce complete regression of metastatic renal cancer in young mice (2–3 mo old; Murphy et al., 2003). As this is roughly equivalent to treating teenage to college-age individuals, we wanted to ascertain whether this IT regimen can be applied to the human cancer scenario with regard to age, so we investigated whether this IT regimen was efficacious in induction of anti-tumor effects in aged tumor-bearing recipients. However, when we treated aged (>16 mo of age) tumor-bearing mice, all the mice rapidly succumbed to the IT within 2 days of regimen administration (unpublished data). To further investigate the IT-induced toxicities with age, we assessed the effects of IT in nontumor-bearing aged mice with anti-CD40/IL-2 IT to ascertain if this rapid mortality was intrinsically related to the age of the recipients. As before, this regimen resulted in a marked and rapid lethality within 2 d of treatment (Fig. 1 A), whereas no mortality was observed in young adult mice.

Necropsy of the aged recipients indicated multiorgan pathologies in response to IT. Aged mice developed marked histopathological changes to the liver (Fig. 1 D), lungs (Fig. 1 E), and gastrointestinal tract (Fig. 1 F) shortly after IT with periportal lymphocytic aggregates in the liver (Fig. 1 D), peribronchiolitis in the lung (Fig. 1 E), and intramucosal lymphocytic aggregates in the gut (Fig. 1 F) compared with their young counterparts. The livers of aged IT-treated mice demonstrated extensive patchy piecemeal necrosis throughout the entire liver (Fig. 1 D). Intestines of aged treated mice showed chronic acute segmental enteritis with extensive mucosal damage, loss of normal villi, and ulceration associated with acute cryptitis (Fig. 1 F). Interestingly, untreated aged mice revealed a preexisting state of mild inflammation even before IT (Fig. 1 C) that was not present in young mice (Fig. 1 B).

We also assessed the effects of other IT regimens. Comparable age-related effects on pathology and serum alanine aminotransferase (ALT) were also observed when aged mice were treated with an IL-2/IL-12 IT regimen (Fig.1, G and H), previously demonstrated to induce potent anti-tumor effects in young mice (Wigginton et al., 1996, 2001). These data indicate that the dramatic induction of a cytokine storm, resulting in multiorgan pathology and correlating with age after systemic immune stimulation, span a variety of regimens.

We then delineated as to when the mice developed this sensitivity to IT. Using aged (>16 mo old) mice, anti-CD40/IL-2 IT resulted in a marked and rapid lethality within 2 days of treatment (Fig. 2, A and B). Significantly increased mortality from anti-CD40/IL-2 was also observed in mice as young as 9 mo (middle-aged; Fig. 2, C and D). However, 6-mo-old mice treated with the same regimen of anti-CD40/IL-2 survived the entire IT regimen, indicating that this was the cutoff for the heightened sensitivity (unpublished data). We have also observed similar results in survival, cytokine production, and pathology in aged BALB/c mice comparable to C57BL/6 data presented in Figs. 1 and 2, suggesting that IT-induced toxicities and mortality were strain independent (not depicted).

Mortality from anti-CD40 and IL-2 was only observed after combination therapy, as mice receiving either agent singly survived the full IT regimen. IL-2 and anti-CD40 monotherapy led to an increase in serum IFN-γ and TNF, respectively, compared with the control group; however, these cytokine levels were 7-fold lower for IFN-γ and 50-fold lower for TNF than the combination of anti-CD40/IL-2 (not depicted).

This increased pathological response to IT was not limited to the anti-CD40 and IL-2 regimen. In addition to this IT, aged mice treated with LPS, to mimic a systemic infection (Munford, 2006), yielded similar heightened pathology as they also succumbed to LPS toxicity more rapidly (Fig. 2 E) than young mice. These data demonstrate that strong systemic immune stimulation results in a lethal reaction that correlates with increased age.

The multiorgan pathology (Fig. 1) and increased mortality (Fig. 2, A–D) in aged mice that received anti-CD40/IL-2 IT correlated with markedly increased serum levels of the proinflammatory cytokines TNF, IL-6, and IFN-γ (Fig. 2, F–I). The levels of TNF, IL-6, and IFN-γ after IT also directly correlated with increasing age (Fig. 2, F–I). This cytokine storm associated with aging was not limited to IT, aged mice treated with LPS not only succumbed to LPS toxicity more rapidly (Fig. 2 E) but also demonstrated higher serum levels of TNF and IL-6 compared with younger mice (Fig. 2 J). Heightened serum levels of ALT, indicative of liver damage, were observed in both treated aged (Fig. 2, K and L) and middle-aged (Fig. 2, M and N) mice.

We then compared the inflammatory cytokine levels both in the serum in and in the tissues. IT with anti-CD40/IL-2 resulted in marked increases in both the serum protein (Fig. 3, A–C) and mRNA levels (Fig. 3, D–F) of TNF, IL-6, and IFN-γ within the tissues of the liver, gut, and lungs compared with younger mice. Increase in TNF expression was the highest in the livers of aged mice, whereas IL-6 expression was most increased in the gut and IFN-γ was elevated in all three organs, suggesting that different proinflammatory cytokines may play a more predominant role in a particular organ system. These results demonstrate that the IT-induced mortality and pathology in aged but not young mice is associated with marked induction of proinflammatory cytokines affecting multiple organs correlating with the increased lethality.

We have previously demonstrated that the anti-tumor effects of anti-CD40/IL-2 IT were mediated by marked expansion and activation of CD8 T cells, although NK cells also expanded after treatment (Murphy et al., 2003). CD8 T cells have also been shown to be the principal anti-tumor mediators of IL-2/IL-12 regimens (Wigginton et al., 2001). To determine the immune cells responsible for the toxicities occurring in aged mice after IT, aged mice were first depleted of T cells (using anti-CD4 and anti-CD8 mAbs), NK cells (using anti-NK1.1), or macrophages (with prior treatment with liposomal clodronate [LC]) followed by anti-CD40/IL-2. The absence of CD4 and/or CD8 T cells or NK cells in aged mice all resulted in comparable IT-induced mortality, organ damage (Fig. 4, A and B), and cytokine induction (not depicted). However, macrophage depletion in aged mice resulted in significant and marked protection from IT-induced toxicities. Interestingly, improvement of pathology was primarily observed in the liver (Fig. 4, C and D) and not in the other organs, indicating that liver pathology was pivotal for the rapid mortality due to the cytokine storm. Macrophage depletion by LC in aged mice was also accompanied by a significant decrease in serum ALT (Fig. 4 E) and proinflammatory cytokines (TNF, IL-6, and IFN-γ; Fig. 4, F–H), and resulted in 100% survival after IT (Fig. 4 I). Depletion of peripheral macrophages was ascertained by flow cytometry (Fig. 4 J). Peritoneal lavage cells recovered from aged mice that were also macrophage-depleted demonstrated significantly lower TNF production upon LPS stimulation, which further demonstrated macrophages as the primary source of proinflammatory cytokines (Fig. 4 K). These data indicate that macrophages, and not lymphocytes, are the major cell type responsible for the IT-related toxicities in aged mice, and that the liver was the principal target organ responsible for mortality.

To further examine the impact of age on the extent of cytokine production by macrophages, BM-derived macrophages (BMDMs) from young and aged mice were isolated and stimulated with LPS. Macrophages from aged mice produced significantly higher TNF and IL-6 compared with young mice (Fig. 5 A). Similarly, human PBMCs, derived from 37 healthy donors ranging from 28 to 95 years old which were differentiated into macrophages in vitro (Zhang et al., 2008) and then stimulated with LPS, revealed a striking age-dependent increase in their ability to produce TNF (Fig. 5, B and D) and IL-6 (Fig. 5, C and E), suggesting that aging (or variables associated with aging) contributes to the increased proinflammatory status of macrophages. The data further suggest that targeting of macrophages may be a potential therapeutic option for systemic immune stimulation, either induced by cancer therapies or during acute sepsis, particularly in the elderly.

Given the strong correlation of proinflammatory cytokine levels with pathology in the aged mice, we next sought to examine their role in the age-dependent toxicities observed after IT. Macrophage depletion, which allowed for protection from acute organ failure and lethality in the aged, led to significant decreases in TNF and IL-6 expression in particular. Pathological TNF and IL-6 expression has been implicated in various systemic inflammatory conditions (Hack et al., 1989; Gantner et al., 1995; Leon et al., 1998; Taylor and Feldmann, 2009; Krüttgen and Rose-John, 2012). We focused on TNF in these next studies as opposed to other elevated cytokines because of its involvement in a variety of systemic pathological conditions, as well as its pleiotropic effects on other cytokines including IL-6 and IFN-γ, which have been shown to be elevated after IT as well (Boccoli et al., 1990; Blay et al., 1992; Vonderheide et al., 2007). Furthermore, TNF is known to amplify IL-6 production (Shalaby et al., 1989; Sheron et al., 1990; Aggarwal, 2003); therefore, we reasoned that TNF inhibition might account for reductions in other inflammatory cytokines. To test this hypothesis, we treated aged WT and aged TNF KO, as well as aged IFN receptor (IFNR)–KO mice with IT, and observed that aged TNF-KO mice were able to survive the entire IT regimen (Fig. 6 A), whereas 50% of the IFNR-KO mice succumbed to IT by day 12 of anti-CD40/IL-2 administration (Fig. 6 A). This indicated a partial involvement of the IFN-γ pathway in toxicities of anti-CD40/IL-2, but that lethality in the aged is predominately dependent on TNF. Aged TNF-KO mice also demonstrated diminished serum levels of IL-6 (Fig. 6 B) as well as the expected lack of TNF (Fig. 6 C), indicating that TNF was at least partially responsible for inducing IL-6 in the cytokine storm. Interestingly, serum IFN-γ levels were increased in aged TNF-KO mice compared with aged WT mice (Fig. 6 D), whereas serum ALT levels were significantly decreased in aged-treated TNF-KO mice (Fig. 6 E). TNF-KO mice given IT demonstrated a significant decrease in hepatic necrosis (Fig. 6, F and G) and serum ALT (Fig. 6 H). These findings suggest that TNF plays a pivotal role in the induction of IT-mediated mortality and, in particular, liver damage.

Several TNF blockade therapies, including chimeric (i.e., Infliximab) and humanized monoclonal antibodies (i.e., Adalimumab) or a human TNF-R IgG 1 fusion protein (i.e., etanercept), are successfully used for the clinical management of inflammation and to minimize autoimmune disorders such as rheumatoid arthritis, Crohn’s disease, ulcerative colitis, psoriasis, and ankylosing spondylitis (Taylor and Feldmann, 2009; Taylor, 2010; Schett et al., 2011). Due to exciting results using TNF-KO mice, we were enthusiastic that TNF blockade for the amelioration of cytokine storm–induced toxicities in the aged may be readily translatable using preexisting, clinically approved treatment options. To test this hypothesis, we assessed the effects of TNF antagonists on IT-mediated toxicities using etanercept (Enbrel). Although etanercept contains a human TNF receptor, murine and human TNF share an 80% homology and etanercept has been shown to decrease TNF-mediated inflammation in mice (Grounds et al., 2005; Hodgetts et al., 2006; Hutchison et al., 2008; Surguladze et al., 2009; Nemoto et al., 2011). To test this hypothesis, aged mice were treated with etanercept, which resulted in significant increases in survival after anti-CD40/IL-2 IT. TNF blockade with IT allowed for greater survival, as 50% of aged mice survived the IT regimen when it was combined with TNF blockade (Fig. 7 A). This enhanced survival correlated with significant improvement in liver pathology (Fig. 7, B and E) in mice receiving combination treatment (IT/etanercept), which was concordant with decreases in serum ALT (Fig. 7 F). Interestingly, no differences were observed in the gut and lung pathology (Fig. 7, C–E), regardless of TNF blockade in the aged mice, further demonstrating the pivotal role of TNF in mediating hepatic changes in aged mice after IT and also demonstrating that the liver was the primary cause for mortality after IT. Interestingly, at the dose administered, etanercept only offered minimal protection in conjunction with the high-dose IT regimen (unpublished data).

In agreement with the TNF-KO data, serum cytokines were also affected after TNF blockade as IL-6 levels were diminished (Fig. 7 G). The induction of IFN-γ in aged mice was not inhibited by TNF blockade (Fig. 7 H). This may be important as it suggested that IFN-γ–dependent anti-tumor effects may still be preserved, as we have previously demonstrated that anti-tumor effects associated with anti-CD40/IL-2 in young mice are IFN-γ–dependent (Murphy et al., 2003). Moreover, serum TNF was diminished after etanercept but there were no significant differences in TNF production with or without TNF blockade (Fig. 7 I), as this drug only antagonizes mechanism of action of TNF.

Furthermore, we have noticed that TNF ablation using TNF-KO mice or etanercept led to marked reductions in IL-6 (Fig. 6 B and Fig. 7 G), suggesting that TNF may also mediate toxicity through modulation of IL-6 levels. To address this, we treated aged mice with IT with or without an IL-6 blocking antibody or with etanercept. Both TNF blockade and anti–IL-6 resulted in lower serum IL-6 and TNF (Fig. 7 K), yet that protection from liver pathology in aged mice was only observed when IT was combined with TNF blockade and not anti–IL-6 (Fig. 7 L). These data indicate that TNF blockade may be of use to ameliorate toxicities in aged tumor-bearing recipients after IT and possibly allow for anti-tumor effects to be maintained.

Because of TNF’s contradictory roles in the suppression and promotion of tumor progression (Carswell et al., 1975; van Horssen et al., 2006; Calzascia et al., 2007; Sethi et al., 2008; Balkwill, 2009), it was imperative to determine whether IT-induced TNF, although critical to generation of systemic toxicities, may also be necessary for anti-tumor responses. Therefore, we next sought to ascertain if IT could be administered in aged tumor-bearing mice in combination with etanercept to prevent IT-associated mortality while preserving the anti-tumor effects induced by IT. Aged mice bearing the 3LL Lewis lung carcinoma were treated with anti-CD40/IL-2 IT and continuous etanercept administration. As observed earlier, aged tumor-bearing mice that received IT alone died very rapidly from acute toxicity compared with aged mice receiving tumor alone (Fig. 8 A). In contrast, aged tumor-bearing mice receiving continuous etanercept administration demonstrated 100% survival during an entire course of IT (12 d) and also resulted in significant anti-tumor effects with increased survival compared with mice receiving tumor alone (Fig. 8 A; death determined due to tumor upon necropsy, not depicted). This combination approach also resulted in CD8 T cell expansion in the spleens of aged mice (Fig. 8 B), as well as preservation of CD8 T cell lytic ability (Fig. 8 C) comparable to what was observed in young recipients (Murphy et al., 2003). These data indicate that TNF blockade allowed for aged tumor-bearing mice to receive effective IT resulting in increased survival, lessened toxicity, and preservation of anti-tumor responses.

Cancer IT has been shown to elicit successful anti-tumor responses both preclinically and clinically (Dougan and Dranoff, 2009). However, cytokine and antibody therapies can also lead to severe and systemic toxicities resulting in cessation of IT. Aging is associated with increased inflammation, potentially rendering cancer patients more susceptible to these toxicities. The mechanisms of increased “inflammaging” are not well understood and the majority of preclinical studies testing new immunotherapies have been investigated using young mouse models. Given that the mean age of a cancer patient is greater than 55 years old, these mouse models do not reflect the potential profound immune changes occurring that result in immune senescence and normal aging.

In the current study, we compared the effects of agonistic anti-CD40 and IL-2, as well as other immunostimulatory regimens, on systemic toxicities in young and aged mice. Our results demonstrate a pronounced age-dependent susceptibility to multiorgan toxicities after systemic immune stimulation resulting from a macrophage-mediated cytokine storm. We also show that aging results in increased inflammatory cytokine production leading to rapid mortality. Our data confirm that the fundamental process of inflammaging may serve as a predisposition to toxicities with age, indicating that application of systemic immune stimulation in the elderly must proceed with caution and demonstrating that increased susceptibility to toxicities from infectious agents may also result.

The rapid onset of mortality coupled with multiorgan tissue damage after IT in aged mice suggested that lethality may be associated with a systemic pathology similar to that experienced after sepsis or shock-like syndromes termed MODS (multiple organ dysfunction syndromes). Aged mice exhibited higher serum levels of proinflammatory cytokines, in particular TNF, IL-6, and IFN-γ, upon anti-CD40/IL-2 stimulation as well as after LPS treatment compared with young mice. We observed similar trends in organ pathology and serum liver enzymes in aged mice receiving IL-2/IL-12 IT as well. Although the aged mice did not succumb to IL-2/IL-12 treatments, they displayed (even at day 11 of therapy) increased systemic toxicities and multiorgan pathology as compared with young-treated mice. However, organ histopathology, although elevated in aged IL-2/IL-12 mice, was slightly lower than what was observed in aged mice treated with anti-CD40/IL-2, which could be indicative of the reasons that IL-2/IL-12–treated mice did not die. Additionally, we have also noted marked differences in histopathology on day 2 versus day 11 in young mice, and given that the mice treated with IL-2/IL-12 survived too and were analyzed for histopathology on day 11, the later time point may also contribute to the overt differences in pathology observed in IL-2/IL-12 mice. Overall, these data suggest that systemic toxicities are not anti-CD40/IL-2 specific but also occur with other cytokine therapies and with a different extent of fatality.

Given the plethora of recent data highlighting the role of microbiota in toxicity and disease (Arthur et al., 2012; Hooper et al., 2012; Gallimore and Godkin, 2013; Kamada et al., 2013), it begs the question as to the role of differential microbiota among institutional animal facilities in our studies. Importantly, in this study, given that the work presented here was performed across multiple organizations and across multiple strains of mice, all three (anti-CD40/IL-2, LPS, and IL-2/IL-12) immunomodulatory regimens resulted in similar patterns of toxicity and 100% mortality by day 2 of therapy (for anti-CD40/IL-2) in aged mice across all institutions. This suggests that the systemic toxicities observed in aged mice are independent on the animal housing conditions and any potential discrepancies that might arise from cleanliness of the animal facility or type of feed, all of which could affect intestinal microbiota.

The aged recipients not only produced higher levels of proinflammatory cytokines in circulation but also within the tissues where the damage was occurring. This was rapid, as death occurred within 2 d in aged mice. Interestingly, even mice as young as 9 mo succumbed to the toxicities. The lifespans of mouse and man are dramatically different. The average laboratory mouse lives 2–3 yr, whereas the average human lives ∼80 yr. As the vast majority of mouse cancer studies use mice starting at 2–3 mo of age, this would be roughly equivalent to treating an adolescent or young adult patient whose immune system is markedly different than an individual over the age of 55, the average age at which cancer is diagnosed and subsequently treated. Therefore, to more accurately reflect the typical cancer patient in the clinic, our data suggest that it may be more beneficial to perform preclinical studies in aged mice, particularly when attempting to accurately model toxicities.

In the immune cell depletion experiments, it was observed that whereas T cells are the predominant tumor effector cell, the systemic cytokine storm and mortality in aged mice were all dependent on macrophages. This age-associated dysregulation in macrophages was similar in humans, as it was observed that macrophages from both aged mice and humans exhibited heightened TNF and IL-6 production after LPS stimulation compared with macrophages from young mice or younger healthy donors.

The critical role for TNF is at least a partial mediator of these effects, as was demonstrated by the TNF-KO mice receiving IT exhibiting decreased serum IL-6, TNF, liver enzymes (ALT), and having preferential protection from liver pathology. In agreement with our data, mice deficient to either TNF or TNF receptors are less susceptible to endotoxic shock from high-dose LPS challenge and increased survival as opposed to WT mice (Smith et al., 1994; Paludan, 2000; Rosas et al., 2001; Kawa et al., 2010). Moreover, both liver enzymes and serum IL-6 were much lower after TNF blockade in our studies. This decrease in proinflammatory cytokines is likely a major contributor to the enhanced survival as well as diminished gastrointestinal and liver pathology. Although, IL-6 is well known as a hepatoprotective cytokine (Cressman et al., 1996), other studies have shown that long-term IL-6 exposure induced SOCS3 (suppressor of cytokine signaling 3) expression in hepatocytes, resulting in exacerbated liver injury (Senn et al., 2003; Rotter Sopasakis et al., 2004; Jin et al., 2006). Other reports have indicated that both IL-6 (Chen et al., 2009) and TNF (Korngold et al., 2003) mediate damage as a result of graft-versus-host disease (GVHD) after allogeneic hematopoietic stem cell transplantation. Interestingly, GVHD studies also suggest that different proinflammatory cytokines may play a more predominant role in a particular organ, although they may all contribute to the overall pathology. Our studies would support that TNF appears to be a primary mediator of hepatic damage after IT, whereas it is likely that other cytokines such as IL-6 may play a more predominant role in gut pathology. It is clear from these studies that liver failure is likely the principal cause of mortality after IT in aged mice.

The anti-tumor responses of anti-CD40/IL-2 are both CD8 T cell and IFN-γ mediated, as previously demonstrated (Murphy et al., 2003). In the current study, we have found that aged mice treated with anti-CD40/IL-2 and TNF blockade were able to mount effective anti-tumor responses against preexisting tumors. Not only did we see protection in the aged mice from IT-induced lethality, we also observed expansion of CD8 T cells and elevated IFN-γ levels using a lower dose of IT with etanercept and the induction of anti-tumor effects. The role of TNF in cancer is complex as it can both promote tumor progression and affect innate immune activation (Sethi et al., 2008). It is possible that the relatively short administration of TNF blockade during IT outweighs any tumor-promoting effects it can induce and the amelioration of toxicities allows for immune activation to manifest in anti-tumor effects.

Clinically, TNF blockade, in addition to being used to treat autoimmune diseases, is used as a treatment for immune-related adverse events (irAEs), particularly colitis, experienced after certain immunotherapeutic cancer regimens such as CTLA4 blockade (Minor et al., 2009). Therefore, there is precedent for its use during anti-cancer therapy. In these patients, however, treatment with the primary IT is halted due to irAE severity and anti-TNF therapy is administered afterward. Anti-tumor immunity is often maintained in these patients, further supporting the concept that TNF may not be essential to anti-tumor immunity and its blockade does not impede tumor immunity. In contrast to this clinical scenario, we show here that IT perhaps need not to be halted, but application of anti-TNF therapies (and in combination with inhibition of other cytokines such as IL-6) can be administered concurrently to alleviate toxicities while not adversely affecting anti-tumor responses.

It will be of particular interest to ascertain whether the increases of these proinflammatory cytokines associated with aging also occur after other cytoreductive insults such as chemotherapy and radiation therapy. Age, outside of frailty, may also play predisposing roles in other disease states, such as infectious disease, and toxicities, such as GVHD after allogeneic hematopoietic stem cell transplantation, due to the heightened proinflammatory state. Thus, aging strongly promotes inflammatory responses in both mouse and man, which can result in multiorgan pathologies after immune stimulation. This inflammatory sensitivity may predispose individuals after infection as well as cytoreductive cancer therapies to adverse events, but interventions affecting the cell types responsible (macrophages) or the inflammatory cytokines (TNF) themselves represent viable options. These studies underscore the importance of considering age as an important variable in the assessment of potential immunotherapies where the target population is predominantly aged.

Female young (2–4 mo old), middle-aged (9–12 mo old), or aged (16–22 mo old) C57BL/6 or BALB/c mice were purchased from Charles River or from the animal production area at the National Cancer Institute. C57BL/6-TNF-KO young (4 mo old) or aged (16 mo old) mice, or C57BL/6–IFNR-KO aged mice (16 mo old) and their age-matched control WT-C57BL/6 were purchased from The Jackson Laboratory. Mice were housed in the animal facilities at the University of Nevada, Reno, the University of California, Davis, or the National Institute on Aging (NIA) at the National Institutes of Health under specific pathogen-free conditions. In each experiment, the young and aged mice were housed in the same animal facility. Animal studies were approved by the University of Nevada, Reno, the University of California, Davis, and the NIA, Baltimore campus Institutional Animal Care and Use committees.

3LL Lewis lung carcinoma was purchased from the American Tissue Culture Collection. Cells were cultured in complete RF10 containing RPMI1640 medium supplemented with 10% FBS, 1% penicillin/streptomycin, 1% (2 mM) glutamine, 1% (1×) nonessential amino acids, 1% (1 mM) sodium pyruvate, 1.5% (15 mM) Hepes, and 1% (5 × 10⁻⁵ M) 2-mercaptoethanol at 37°C in a humidified atmosphere containing 5% CO₂. Cell viability was checked by trypan blue and counted with a hemocytometer. 3LL cells at 2.5 × 10⁵ cells were suspended in 0.1 ml PBS and injected i.v. into young or aged C57BL/6 mice, and 3 d later IT was initiated.

The agonistic anti–mouse CD40 antibody (clone FGK115B3) was generated via ascites production in our laboratory as previously described (Murphy et al., 2003). The endotoxin level of the anti-CD40 was <1 endotoxin unit/mg antibody as determined by a quantitative chromogenic limulus amebocyte lysate kit (Lonza). Recombinant human IL-2 (rhIL-2; TECIN Teceleukin; Roche) was provided by the National Cancer Institute (NCI). Recombinant mouse IL-12 (PeproTech) was purchased from commercial vendors. Etanercept (Amgen and Pfizer) was provided by E. Maverakis. Some mice received human or rat IgG (Jackson ImmunoResearch Laboratories, Inc.) as a control for etanercept or anti-CD40 treatments, respectively. In some experiments, NK cells were depleted using 300 µg anti-NK1.1 (PK136) grown by the National Cell Culture Center. CD8⁺ T cells were depleted using 500 µg of the rat antibody to mouse CD8 (clone YTS169.4) produced in ascites, and the endotoxin level was 3.6 EU/mg antibody. CD4⁺ T cells were depleted with an anti-CD4 antibody at 500 µg (clone GK1.5; gift from G.B. Huffnagle, University of Michigan, Ann Arbor, MI). All antibodies were injected i.p., except etanercept which was injected subcutaneously.

Mice were treated with agonist anti-CD40 antibody and rhIL-2 as previously described (Murphy et al., 2003). In brief, anti-CD40 was administered daily for a total of 5 consecutive days (day 0 to 4) and IL-2 was administered twice a day for a total of 4 d (days 1, 4, 8, and 11). Control mice received rat IgG (Jackson ImmunoResearch Laboratories, Inc.) and PBS (Cellgro). Survival was monitored daily. A high dose or low dose of anti-CD40/IL-2 was used and is described in figure legends and further specified below.

Mice received 80 µg of agonist anti-CD40 and 10⁶ IU IL-2 in 0.2 ml PBS i.p. Control mice received 80 µg rIgG and PBS.

Mice received 40 µg of agonist anti-CD40 and 2.5 × 10⁵ IU IL-2 in 0.2 ml PBS i.p. Control mice received 40 µg rIgG and PBS.

In some experiments in which TNF was blocked, etanercept was administered subcutaneously at 1.5 mg/0.2 ml PBS in aged mice. Etanercept was administered on days −1 and 1 for experiments when mice were scarified at day 2 of anti-CD40/IL-2 therapy. In survival from systemic toxicities and anti-tumor studies, etanercept was administered on days −1, 1, 3, 7, and 9. Tumor cells were injected i.v. on day −3 with day 0 being the start of anti-CD40/IL-2 treatment.

To block IL-6, aged mice received a rat monoclonal antibody (CNTO 345) specific for mouse IL-6 (Centocor Research and Development Inc.) at 1.0 mg/0.2 ml in PBS on day −1 before the start of anti-CD40/IL-2 IT treatment on day 0. Mice were scarified at day 2 of IT for serum cytokine measurements and liver pathology.

Recombinant mouse IL-12 at 0.5 µg/0.2 ml was administered to BALB/c mice i.p for 5 consecutive days (says 0 to 4) during week 1 and for another 4 consecutive days during week 2 of IT (days 7 to 11). RhIL-2 at 3 × 10⁵ IU/0.2 ml was administered i.p twice a day, on days 0, 4, and 7.

Macrophages were depleted in vivo using LC (Encapsula Nano Sciences) and administered on days −2 and 0 for experiments requiring euthanasia on day 2 or on days −2, 0, 2, and 4 for survival studies. Day 0 is the start of anti-CD40/IL-2 treatment, which is descried in the above section for the schedule of anti-CD40/IL-2 therapy. Clodronate or control-loaded liposomes were injected at 0.2 ml per dose i.p. 95% of macrophages were depleted and this was verified by staining for flow cytometry for CD45⁺ (Pacific blue), CD19⁻ (PE), CD11b⁺ (APC-Cy7), and F4/80⁺ (APC) cells in the spleen and peritoneal lavage.

Young, middle-aged, or aged C57BL/6 mice received a single 0.2 ml i.p injection of either PBS or LPS derived from Escherichia coli serotype 055:B5 (Sigma-Aldrich) resuspended in PBS at doses between 1.5 mg/kg body mass. Mice were examined continuously for survival experiments.

PBMCs were collected from healthy young or aged donors with written informed consent in accordance with the IRB-approved human subject protocol #2003054 of the Clinical Research Branch, National Institute on Aging. PBMCs from aged subjects were also collected from participants in the National Institute on Aging Baltimore Longitudinal Study of Aging (BLSA), approved by the IRB, and all participants signed informed consent. Details of the BLSA recruitment and testing methodology are described elsewhere (Shock et al., 1984). Human PBMCs were obtained by Ficoll-Hypaque density centrifugation after which monocytes were purified from PBMCs using the human Monocyte Isolation kit II (Miltenyi Biotec). Isolated monocytes were typically >94% after isolation. Monocytes were either directly cultured in AIM-V serum-free media (Invitrogen) on poly:IC-coated plates and stimulated with 50 ng/ml human recombinant macrophage CSF (hM-CSF; GenScript USA Inc.) for 6 d, washed, and recultured in AIM-V with hM-CSF and 0.5% participant plasma for an additional 3–4 d. The purity of the cultured human macrophage generated was >92% based on flow cytometric analysis and/or Giemsa/nonspecific esterase staining. Macrophages isolated from these cultures were harvested using TrypLE Express Stable Trypsin-Like Enzyme with Phenol red (Life Technologies) and gently scraping with a rubber policeman. Cells were washed and plated on poly:IC-coated plates and stimulated with 50 ng/ml LPS for 48 h, and then the supernatants were collected to evaluate cytokine expression.

Murine BMDMs were isolated from the femurs of young and aged C57BL/6 mice as previously described (Zhang et al., 2008). BM cells were suspended, counted, and cultured on tissue culture plates precoated with poly:IC using a BM culture media containing DMEM (Invitrogen), 10% heat-inactivated fetal calf serum, 2 Mm l-glutamine, 100 U/ml penicillin, 100 ng/ml streptomycin, 20% L929 (American Type Culture Collection no. CCL-1)–conditioned medium, and 100 ng/ml hM-CSF for 6 d at 37°C in 10% CO₂. In certain experiments, BM cells were enriched for murine monocytes before culture using EasySep Mouse Monocyte Enrichment kit (STEMCELL Technologies). After 6–7 d, macrophages were removed by treatment with TrypLE Express Stable Trypsin-Like Enzyme with Phenol red and gently scraping with a rubber policemen. The cells were isolated, cultured, and stimulated with 50 ng/ml LPS for 24 h, and then the supernatants were collected to evaluate cytokine expression. Macrophage purity was found to be >94% live macrophages as assessed by staining with anti–CD11b-PE and anti–F4/80-FITC (BD).

Serum levels of TNF, IFN-γ, and IL-6 were quantified by multiplex measurement using the Cytometric Bead Array CBA (BD) kit according to manufacturer’s instructions. Each sample was run in triplicate. Upon analysis of raw data, the MFIs in the detection reagent channel of each bead cluster were quantified. Serum cytokine concentrations were then extrapolated relative to a standard curve created by serial dilution of multiplexed mouse standard cytokines run in parallel. Data were acquired on a Fortessa cell analyzer using FACSDiva software (BD) and analyzed using FlowJo software (Tree Star). Standard regressions and sample statistical significance was determined using Prism data analysis software (GraphPad Software).

For certain studies, human and murine cytokines were analyzed in culture supernatants using Bio-Plex Mouse and Human Cytokine Singleplex kits according to the manufacturer’s instructions (Bio-Rad Laboratories).

The concentration (units per liter) of serum ALT in blood was quantified using the ALT Enzymatic Assay kit (ID Labs, Inc.) according to manufacturer instructions. Colorimetric determination of ALT levels was performed by reading of absorbance of each well at 340 nm on a VERSAmax Tunable Plate Reader (Molecular Devices) and data were collected using SOFTmax PRO software (Molecular Devices). Dilutions of the pyruvate control, included in the kit, were used to construct a standard curve to calibrate the assay. Serum samples were assayed in triplicate.

Liver, lung, and whole intestines were collected on day 2 of IT, flushed and fixed in 10% paraformaldehyde, embedded in paraffin, cut in sections, and stained with hematoxylin and eosin (H&E). All tissues were prepared and stained at the Histology Consultation Services, Inc. in Everson, WA. Images were captured with a BX4 microscope (Olympus) equipped with a Q-color3 camera and 10× numerical aperture objective lens. Magnification for each captured image is specified for each experiment in the figure legend. Grading of histopathological inflammation was performed using a grading scale from 0 to 4 in a blind fashion by a board-certified pathologist. Grading score criteria of tissue inflammation and necrosis ranged from 0 to 4, with 0 = no inflammation, 1 = minimal/intermediate, 2 = mild, 3 = moderate, and 4 = severe with tissue necrosis. This grading score for liver, lung, and gastrointestinal tract was consistent with the previously published grading systems (Yousem et al., 1996; Anonymous, 1997).

Total RNA from mouse tissues was isolated using RNeasy mini kit (QIAGEN). RNA quantities were standardized across samples with a maximum of 1 µg of total RNA reverse transcribed using a high capacity cDNA reverse transcription kit (Applied Biosystems) containing RT buffer, a random primer, reverse transcription, and RNase inhibitor. RNA was transcribed for 60 min at 37°C, for 5 min at 95°C, and then for 5 min at 4°C using AB Veriti Therma Cyler (Applied Biosystems) with 96-well Aluminum Sample Block Module.

Quantitative real-time PCR was performed using AB Step-ONE Plus (Applied Biosystems) in the presence of SYBR Green Supermix (Applied Biosystems). Primer assays for TNF, IFN-γ, and IL-6 were purchased from QIAGEN. mRNA levels were calculated using the comparative threshold cycle method (C_t). C_t values for the housekeeping gene (GAPDH) and for the genes of interest were determined, and the difference between the C_t values of each gene of interest and the mean GAPDH Ct was calculated (ΔC_t). Differences in ΔC_t (ΔΔC_t) of genes of interest in treatment groups (anti-CD40/IL-2) were normalized to control groups (rIgG/PBS) as shown in the following equation: ΔΔC_t = ΔC_t(sample) − ΔC_t(mean of control group). RT-PCR data are presented as fold change expression = 2^−ΔΔCt of each cytokine in comparison to control groups (rIgG/PBS).

10⁶ cells from single cell suspensions from spleen or peritoneal lavage were first incubated with Fc block (BD) and then labeled with anti–mouse antibodies, including FITC anti–mouse CD3 (clone 145-2C11), AF700 anti–mouse CD8 (clone 53–6.7), Pacific blue anti–mouse CD45 (clone 30-F11), APC anti–mouse F4/80 (clone BM8), APC rIgG2a (clone RTK2758), APC-Cy7 anti–mouse CD11b (clone M1/70), and PE anti–mouse CD19 (clone 1D3). Anti–mouse CD19 was purchased from BD. All other antibodies were purchased from BioLegend. Listmode data files were collected using a Fortessa cell analyzer with FACSDiva software (BD). All datasets were analyzed using FlowJo software.

Splenic CD8⁺ T cells (effectors) from aged mice treated with RIgG/PBS or anti-CD40/IL-2 or anti-CD40/IL-2/Etanercept for 9 d were serially diluted in a 96-well U-bottom plates in RF10c media as previously described (Tietze et al., 2012). P815 cells (targets) were labeled with 100 µCi ⁵¹Cr (NEZ030S; Perkin Elmer) per 10⁶ cells and incubated for 30 min with 1 µg/ml anti-CD3e (eBioscience; clone HIT3a). 10⁴ P815 targets were added to each well at different effector to target (E:T) ratio and incubated at 37°C for 4 h. Supernatants were removed, mixed 1:1 with scintillation fluid, and analyzed on a scintillation counter (Wallac). Maximum release was determined by adding 100 µl 1× Triton X-100 detergent (Sigma-Aldrich) to target cells. Spontaneous release was determined by adding 100 µl RF10c media to 100 µl of target cells. Specific ⁵¹Cr release was calculated as: % lysis = 100% × (experimental − spontaneous)/(maximum − spontaneous).

Statistical analysis was performed using Prism software. Data were expressed as mean ± SEM. For analysis of three or more groups, the nonparametric ANOVA test was performed with Bonferroni’s post-test. Analysis of differences between two normally distributed test groups was performed using the Student’s t test. Welch’s correction was applied to Student’s t test datasets with significant differences in variance.

We thank Monja Metcalf and Weihong Ma for technical help.

This work was supported by grants from the National Institutes of Health (CA0905572 and AG034874) and by the Intramural Research Program of the National Institute on Aging, National Institutes of Health.

The authors declare no competing financial interests.