Transgenic mice have higher Ncf1 expression and oxidative burst in macrophages only.

Since macrophages had the highest capacity to burst as compared with DCs and B cells, macrophages might be important APCs in regulating T cell responses via ROS. To investigate the role of Ncf1 in macrophages specifically, a transgenic mouse was developed, expressing functional Ncf1 restricted to macrophages on an Ncf1 mutant B10.Q background using a human CD68 promoter (B10.Q^MN transgenic mice; MN, macrophage Ncf1) (16). The Ncf1 mutation, originally on a C57BL/6J-m^+/+Lepr^db background, was backcrossed to B10.Q for more than 12 generations, and we could not identify any remaining B6-specific fragments through informative microsatellites in the congenic mouse (4, 17). The mutation in Ncf1 affects splicing and leads to expression of low levels of truncated forms of Ncf1 protein that were not detectable with the FACS staining used (17). To confirm functional expression of Ncf1 due to the transgene, Ncf1 expression was determined by flow cytometry in mice with all genotypes for Ncf1 and positive or negative for the transgene. In the Ncf1 mutated transgenic mice (Ncf1^*/*MN⁺), significantly higher levels of Ncf1 were detected in macrophages (F4/80⁺CD11c^–) from spleen as compared with transgene-negative mice (Ncf1^*/*MN^–), reaching levels comparable to those in Ncf1 heterozygous (Ncf1^+/*) mice. This difference in expression was neither observed in other spleen APCs (DCs [CD11c⁺F4/80^–] and B cells [B220⁺CD11b^–]) nor in T cells, indicating macrophage-specific expression (Figure ​(Figure2A).2A). In neutrophils (Gr1⁺F4/80^–), no differences in Ncf1 expression or burst between transgenic and nontransgenic mice were observed either, indicating that the CD68 promoter did not act in neutrophils (not shown). Functionality of Ncf1 in macrophages from Ncf1^*/* transgenic mice was confirmed by measuring ROS production in spleen macrophages after stimulation with PMA, showing that macrophages from mice expressing the transgene (MN⁺) were indeed able to exert oxidative burst in contrast to those from transgene-negative mice (MN^–) (Figure ​(Figure2B).2B). In Ncf1^+/* mice, a significant difference in Ncf1 expression between MN^– and MN⁺ mice was observed as well, although this did not translate into a significant difference in burst, which might be due to differences in sensitivity or variation in the assays used. In other organs and in blood, similar results were obtained (not shown).

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Figure 2

Transgenic mice show increased Ncf1 expression and burst by macrophages only.

(A) Expression levels of Ncf1 were determined in B10.Q^MN transgenic mice, expressing functional Ncf1 under control of the human CD68 promoter on an Ncf1 mutant (*/*), heterozygous (+/*), or wild-type (+/+) background. Spleen macrophages (F4/80⁺CD11c-) express significantly higher levels of Ncf1 when positive for the transgene (black bars: MN⁺) as compared with transgene-negative mice (white bars: MN^–). This difference in Ncf1 expression was not observed in DCs (F4/80^–CD11c⁺), B cells (B220⁺CD11b^–), or CD4⁺ T cells (CD3⁺CD4⁺). (B) Accordingly, macrophages from Ncf1^*/* transgene–positive (MN⁺) mice were able to exert oxidative burst that was significantly higher than in transgene-negative (MN^–) mice. This difference was not observed in DCs, B cells, or T cells. Mean ± SEM of 4 mice are shown. ^#P < 0.05.

ROS produced by macrophages protect against arthritis.

To determine whether expression of functional Ncf1 restricted to macrophages had an ameliorating effect on arthritis development, arthritis was induced in littermates representing the 6 groups by immunization with collagen type II (CII) to induce CIA. Ncf1 mutant transgenic mice (Ncf1^*/*MN⁺) expressing functional Ncf1 on macrophages only developed significantly less severe arthritis than the Ncf1 mutant, nontransgenic controls (Ncf1^*/*MN^–) (Figure ​(Figure3A).3A). This protective effect was not only observed in the homozygous mutant mice but also in the heterozygous (Ncf1^+/*) mice, arguing for a dose-dependent effect of ROS produced by macrophages on T cell activation. The disease pattern in Ncf1^*/*MN⁺ mice was similar to that in Ncf1^+/*MN^– mice and only increased in severity after boost at day 35 whereas Ncf1^*/*MN^– mice developed severe arthritis soon after immunization, before boost. The difference in severity due to transgenic expression of Ncf1 in macrophages was not observed in the Ncf1 wild-type (Ncf1^+/+) mice, indicating that the effect of the transgene was not dependent on interference with other genes.

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Figure 3

ROS production by macrophages decreases arthritis severity.

(A) Mice expressing functional Ncf1 on macrophages only (Ncf1^*/*MN⁺: filled squares; n = 23) developed significantly less severe CIA as compared with Ncf1^*/*MN^– (open circles; n = 15) mice. After boost at day 35, a similar difference was also observed between Ncf1 heterozygous (+/*) mice with (n = 34) or without (n = 29) the transgene. No differences were observed in Ncf1 wild-type (+/+; n = 21 and 27) mice. All groups were included in each experiment. Mean ± SEM are shown of all mice, run in 2 different experiments with exactly the same setup, with the indicated total number of mice per group. ^#P < 0.05; ^†P < 0.005; ^‡P < 0.0005. (B) Anti-CII IgG levels were determined at 10, 42, and 89 days after immunization and were significantly lower in transgene-positive (MN⁺) Ncf1^*/* mice as compared with transgene-negative (MN^–) Ncf1^*/* mice. Sera from the CIA experiments as shown in A were used, with similar numbers of mice as indicated there. Means ± SEM are shown.

We showed before that Ncf1^+/* and Ncf1^+/+ mice produced lower levels of anti-CII Ab as compared with the Ncf1^*/* mice (4). To determine whether this difference was also present between Ncf1^*/*MN^– and Ncf1^*/*MN⁺ mice, serum was obtained at days 10, 42, and 89 after immunization and assayed for presence of antibodies of different isotypes reactive with CII. As shown in Figure ​Figure3B,3B, the levels of total anti-CII IgG were significantly lower in Ncf1^*/*MN⁺ mice as compared with the Ncf1^*/*MN^– mice at day 42 and day 89. Already at day 10, Ncf1^*/* mice had produced more anti-CII IgG as compared with Ncf1^+/* or Ncf1^+/+ mice, coinciding with the earlier disease onset, although total levels were low compared with the other days. Comparable patterns were observed for the specific subclasses IgG1, IgG2a, and IgG2b, with higher levels of IgG subclasses in Ncf1^*/*MN^– mice at day 43 and less pronounced differences on day 89 (Supplemental Figure 1, A–C; supplemental material available online with this article; 10.1172/JCI31935DS1). The levels of total IgG in serum did not differ between the different genotypes, excluding a direct effect of the mutation in Ncf1 on B cell function (Supplemental Figure 1D). These results suggest differences in T cell help to B cells as a result of a lower ROS production in macrophages.

Ncf1 in macrophages is not important during the effector phase of arthritis.

The observed difference in anti-CII Ab levels might be responsible for the observed difference in arthritis severity in transgenic versus nontransgenic mice. Although we have previously shown that arthritis in both Ncf1 mutant mice and rats is T cell mediated, we wanted to exclude the possibility that functional Ncf1 on macrophages mediated its arthritis-ameliorating effect in the joint during the effector phase, via, e.g., increased levels of anti-CII mAb and subsequent complement activation and FcR interactions. The general belief is that ROS are harmful in the effector phase of arthritis and enhance joint destruction; therefore, one would expect increased disease severity in mice expressing functional Ncf1. To investigate this in a T cell–independent model, arthritis was induced with a cocktail of antibodies directed against 4 different epitopes on CII (C1, J1, U1, C2; collagen antibody-induced arthritis [CAIA]) (18). It was indeed observed that Ncf1^*/* mice had a tendency to develop less severe CAIA (Figure ​(Figure4A)4A) with lower incidence (Figure ​(Figure4B)4B) after LPS injection at day 7, opposite to the pattern observed in CIA. Presence or absence of functional Ncf1 in macrophages did not result in different disease patterns, severity, or incidence. This indicates that Ncf1 in macrophages does not have its major regulatory effect on the effector phase of arthritis in the joints but rather operates through modifying the initiation phase.

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Figure 4

ROS produced by macrophages do not affect the inflammatory phase.

CAIA was induced by injecting 4 mg of a 4 mAb cocktail reactive with CII i.v. into B10.Q^MN mice. LPS was injected 7 days later (day 7). Arthritis severity and incidence were determined over time. Mean ± SEM are shown. No significant differences between transgene-positive or -negative mice were observed for either Ncf1 genotype (Ncf1^*/* MN^–, n = 7; MN⁺, n = 6; Ncf1^+/* MN^–, n = 9; MN⁺, n = 8; Ncf1^+/+ MN^–, n = 6; MN⁺, n = 3).

Mutated Ncf1 in macrophages increases T cell reactivity.

ROS as produced by macrophages might influence T cell response, resulting in the observed difference in arthritis severity and anti-CII IgG levels. To investigate the role of macrophage-derived ROS on T cell activation, we determined T cell responses just after the priming phase but before disease onset. Spleen cells were isolated from mice with the different genotypes 10 days after immunization with pepsin-digested CII (CII) in CFA. Cell suspensions were restimulated in vitro with lathyritic CII (lathCII) to avoid a response against pepsin, and IL-2 production was determined as a measure for T cell activation. As shown in Figure ​Figure5A,5A, IL-2 production was highest in Ncf1^*/*MN^– mice and almost absent in Ncf1^*/*MN⁺ mice. This difference was also observed between Ncf1^+/* mice with or without the transgene. In most experiments, Ncf1^*/*MN⁺ mice even had a tendency to produce lower levels of IL-2 as compared with the other groups, which might be due to differences in CII-specific T cell numbers in the spleens. In the absence of ROS, T cells thus react vigorously on restimulation whereas functional Ncf1 in macrophages significantly diminishes activation. To determine whether this was dependent on increased activation or a higher frequency of activated T cells, IFN-γ ELISPOT assays were conducted. It was shown that fewer T cells from Ncf1^*/*MN⁺ mice produced IFN-γ as compared with Ncf1^*/*MN^– mice when restimulated with lathCII (Figure ​(Figure5B),5B), indicative of decreased responsiveness of the T cells to CII as a result of ROS production by macrophages. In addition, the spot size was significantly smaller in Ncf1^*/*MN⁺ mice as compared with Ncf1^*/*MN^– mice, indicating that the amount of IFN-γ produced was also lower (not shown). Similar results were obtained when inguinal LN cells were used (not shown).

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Figure 5

Mice with mutated Ncf1 in macrophages have more and more active anti-CII T cells.

Spleen cells from B10.Q^MN mice immunized 10 days earlier with CII were restimulated with lathCII, and levels of IL-2 present in the supernatant were measured by ELISA. (A) Ncf1 mutant (*/*) and heterozygous (+/*) transgene-negative mice (MN^–) produced significantly more IL-2 compared with transgene-positive (MN⁺) mice. (B) Cells from the same spleens were subjected to IFN-γ ELISPOT. The number of spots after restimulation with lathCII was significantly lower in transgenic mice. (C) DCs grown from bone marrow with GM-CSF and matured with LPS induced similar amounts of IL-2 production by HCQ10 hybridoma T cells, irrespective of transgene or Ncf1 genotype. (D) In contrast, p-macrophages (pM) from Ncf1^*/*MN⁺ and Ncf1^+/+MN^– mice induced lower levels of IL-2 production by HCQ10 compared with Ncf1^*/*MN^– mice. IL-2 (E) and IFN-γ (F) production after immunization and in vitro restimulation with OVA was higher in Ncf1^*/*MN^– mice compared with Ncf1^*/*MN⁺ and Ncf1^+/+ mice in both spleen and LNs. For A, B, E, and F, means ± SEM of 2 experiments with 3 mice per group are shown. C and D show the results of 1 out of 2 representative experiments each with 4 mice per group. ^#P < 0.05; ^##P < 0.01.

To exclude the possibility that the transgene affected antigen presentation by DCs, DCs were grown from bone marrow from naive mice under GM-CSF stimulation, and DC phenotype was confirmed by FACS (19). DCs were mixed with CII to allow uptake and processing and subsequently stimulated with LPS to induce maturation and upregulation of MHC class II and costimulatory molecules. In Figure ​Figure5A,5A, it is shown that T cell responses did not differ between Ncf1^+/*MN^– and Ncf1^+/*MN⁺ or Ncf1^+/+MN^– mice. For this reason, we only show Ncf1^+/+MN^– mice as controls in this and subsequent experiments. Mature DCs were coincubated with HCQ10 hybridoma T cells, specific for the glycosylated CII epitope 259–270 bound to H2-A^q, and IL-2 production was determined as a measure of T cell activation (20). It was shown that DCs from these mice induced comparable levels of T cell activation, regardless of presence or absence of the transgene (Figure ​(Figure5C).5C). As a control, macrophages were isolated from the peritoneum from naive mice and exposed to CII and HCQ10 T cells. Peritoneal macrophages (p-macrophages) from Ncf1^*/*MN^– mice induced higher levels of IL-2 production as compared with those from Ncf1^*/*MN⁺ mice, which were comparable to IL-2 production induced by Ncf1^+/+MN^– macrophages (Figure ​(Figure5D).5D). No differences in IL-2 production were observed between genotypes in absence of CII (not shown). These data indicate that the transgene only acts in macrophages and excludes a role in DCs.

To determine whether the observed increased T cell response in Ncf1^*/*MN^– mice was restricted to a specific antigen, mice were immunized with OVA instead of CII, and after 10 days, spleens and LNs were harvested. Single-cell suspensions were restimulated with OVA, and subsequently IL-2 (Figure ​(Figure5E)5E) and IFN-γ (Figure ​(Figure5F)5F) production was determined by ELISA and ELISPOT, respectively. Similar patterns were observed as with CII. For spleen, the differences between Ncf1^*/*MN^– and Ncf1^*/*MN⁺ mice were not as big as in the CII experiments but were more pronounced when LNs were used. These data indicate that T cell responses against different antigens are lower when macrophages can produce ROS and are thus not restricted to CII.

Macrophages expressing functional Ncf1 suppress T cell responses in an antigen-dependent way.

To confirm dependence on antigen presentation and to determine whether the increased T cell activation as shown in Figure ​Figure55 was dependent on an increased activation status of the T cells or rather on an increased ability of macrophages to present antigen, the following experiments were performed. CD4⁺ T cells were isolated from spleens from Ncf1^*/*MN^–, Ncf1^*/*MN⁺, and Ncf1^+/+MN^– mice, 10 days after immunization with CII. Macrophages were isolated from the peritoneum of naive mice with the same genotypes. Macrophages and T cells were coincubated in the 9 possible combinations while stimulated with CII, purified protein derivative (PPD), or no antigen. PPD is the immunogenic mycobacterial compound in CFA and is here used as a positive control. This setup allowed us to conclusively state whether the effect of macrophage ROS on T cell activation was mediated via antigen presentation or not. The results confirmed that T cells from mice lacking oxidative burst (due to mutated Ncf1) responded more vigorously in vitro than T cells from mice with functional burst only in macrophages or in all APC types (Figure ​(Figure6A).6A). This was independent of how activation was measured (by proliferation, IL-2, or IFN-γ production). This indicates the processes of T cell selection, maturation, and differentiation in mice with mutated Ncf1 in macrophages are different in comparison to those in mice with functional Ncf1 in macrophages. However, when the effect of macrophages with functional burst on these T cells was addressed, it became clear that these macrophages suppressed the T cell response in vitro, as measured by proliferation and IL-2 but not IFN-γ production. This shows that ROS produced by macrophages also affect antigen presentation in vitro and confirms that macrophages suppress immune responses in vivo by producing ROS. That the IFN-γ production was increased in all conditions with Ncf1^*/*MN^– T cells, regardless of the origin of the macrophages, indicates that IFN-γ production during presentation was not influenced by macrophages but only dependent on the origin of the T cells. Since the only difference between the mice from which the T cells originated was functional Ncf1 in macrophages, this argues for an educational effect of macrophage ROS earlier than during peripheral antigen presentation, e.g., in the spleen or thymus. Conditions stimulated with PPD as a positive control showed similar patterns but with higher responses (Figure ​(Figure6B)6B) whereas all conditions without antigen showed similar low levels of IL-2, proliferation, and IFN-γ production (Figure ​(Figure6C).6C). This indicates that the observed increased response to CII and PPD was antigen dependent, but not restricted to CII.

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Figure 6

Macrophage ROS suppress IL-2 but not IFN-γ production by Ncf1 mutant T cells.

Purified CD4⁺ T cells from CII immunized Ncf1^*/*MN^– (white bars), Ncf1^*/*MN⁺ (gray bars), and Ncf1^+/+MN^– (black bars) were incubated with purified p-macrophages from naive mice from the same genotypes (depicted on the x axes) in all 9 combinations and restimulated with lathCII (A), PPD (B), or nothing (Ctr) (C). IFN-γ production, IL-2 production, and the proliferative response were determined. IFN-γ production was increased in all conditions with Ncf1^*/*MN^– T cells whereas IL-2 production and proliferation were suppressed by macrophages originating from Ncf1^*/*MN⁺ or Ncf1^+/+MN^– mice. Means ± SEM of 6-8 mice per group obtained from 3 different experiments are shown. ^#P < 0.05, ^##P < 0.01.

These experiments were performed in parallel with experiments on naive mouse spleen cells depleted for T cells, allowing both macrophages and DCs to be present in a ratio as occurring in vivo. This setup allowed us to determine whether the suppressive effect of macrophages overshadows the activating potential of DCs as professional APCs. We observed patterns similar to those in Figure ​Figure66 for IL-2 and IFN-γ production as well as for proliferative responses, suggesting that the suppressive effect of Ncf1-sufficient macrophages is dominant over the T cell–activating effect of Ncf1 mutant DCs.

T cell number and phenotype do not differ between genotypes.

The results as shown in Figures ​Figures55 and ​and66 leave room for the possibility that T cells from Ncf1^*/*MN^– mice have higher basal activation levels as compared with Ncf1^*/*MN⁺ or Ncf1^+/+MN^– mice. To investigate this, we measured T cell numbers (CD3⁺CD4⁺ and CD3⁺CD8⁺) and expression of activation markers (CD44 and CD69) on T cells from naive mice or mice immunized 10 days previously. This was done for blood, spleen, thymus, and LNs (the latter only from immunized mice). No differences were found in CD4 or CD8 T cell numbers (shown as CD4/CD8 ratio; Figure ​Figure7A)7A) nor in expression levels of CD44 and CD69 in naive or immunized mice (Supplemental Figure 2A). To determine whether there was a difference in activation threshold of T cells from the different genotypes, spleen cells were stimulated with platebound anti-CD3, anti-CD3 plus soluble anti-CD28, concanavalin A (ConA), or PMA in decreasing concentrations. Results from the highest concentrations are shown (anti-CD3, 10 μg/ml; anti-CD28, 2 μg/ml; ConA, 3 μg/ml; PMA, 50 ng/ml). We measured T cell–specific cytokines IL-2 and IFN-γ and proliferation after 24 hours and 3 days, respectively. No differences in IL-2 production were observed between genotypes (Figure ​(Figure7).7). However, IFN-γ production was significantly higher in spleens from Ncf1^*/*MN^– mice as compared with the other genotypes (Figure ​(Figure7C),7C), similar to the results shown in Figure ​Figure5,5, indicating differences in education. The relatively low levels of IFN-γ upon stimulation with ConA or PMA might be due to the fact that total spleen cells were used in contrast with anti-CD3 stimulation, which is T cell specific. The contrasting high levels of proliferation due to ConA and PMA might be due to proliferation of other cell types as well. The low level of proliferation of Ncf1^*/*MN^– splenocytes upon anti-CD3/28 stimulation might be due to exhaustion of medium due to exaggerated proliferation or another unknown parameter; IL-2 levels are high, as expected, and normally we observe that proliferation follows IL-2 levels. In lower concentrations of anti-CD28 this difference was not as pronounced.

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Figure 7

IL-2 production and proliferation do not differ after T cell stimulation with anti-CD3 or mitogen.

(A) T cell numbers (CD3⁺CD4⁺ and CD3⁺CD8⁺) were measured by flow cytometry in different immune compartments (BL, blood; SPL, spleen; TH, thymus; ILN, inguinal LNs) from naive mice and mice immunized 10 days previously and depicted as CD4/CD8 ratio; there were no differences between the genotypes. (B–D) Stimulation of splenocytes from naive mice with anti-CD3 (10 μg/ml), anti-CD3 plus anti-CD28 (2 μg/ml), ConA (3 μg/ml), or PMA (50 ng/ml) did not result in different levels of IL-2 production or proliferation, but IFN-γ production by Ncf1^*/*MN^– mice was significantly higher compared with Ncf1^*/*MN⁺ or Ncf1^+/+MN^– mice, except for the ConA stimulation. Mean ± SEM are shown from 4 mice per genotype for all conditions, ^#P < 0.05.

When spleen cells from naive mice were analyzed for IL-2 or IFN-γ production upon stimulation with CII, only background levels of these cytokines were observed, and no differences between groups were present (not shown). This confirms that the increased activity of T cells in Ncf1^*/*MN^– mice is only detectable after antigenic stimulation and not a general phenomenon.

In addition, differences in expression levels of MHC class II and costimulatory molecules on macrophages from the different mice might affect T cell activation. Expression levels of MHC class II, ICOSL (CD275), CD80, and CD86 were determined by flow cytometry on macrophages (F4/80⁺CD11c^–) from different immune compartments from naive mice or mice immunized 10 days previously, but no differences were observed (Supplemental Figure 2B).

CIA and CAIA.

CIA was induced by injecting 100 μg of rat CII emulsified in CFA intradermally at the base of the tail (4). After 35 days, mice were boosted with 50 μg of CII in incomplete Freund’s adjuvant. Arthritis development was scored using a macroscopic scoring system: 1 point was given for each swollen or red toe or joint and 5 points for a swollen ankle, adding up to a maximum score of 60 points per mouse. Serum was taken at day 10, day 42, and when sacrificed. CAIA was induced by i.v. injection of 4 mAb directed against different epitopes on CII (C1, J1, D3, and U1) with a total amount of 4 mg. At day 7, 25 μg of LPS was injected i.p., and disease was followed over time (18).

Antibodies and antigens.

The following antibodies were used: F4/80-bio directed against macrophages, N4.18-APCs against CD11c, RA3-6B2-cychrome directed against CD45R/B220, M1/70-FITC directed against CD11b, Rb6-bio against Gr-1, 145-2C11-bio against CD3, H129.9-APCs against CD4, IM7-APCs against CD44, and H1.2F3-APCs against CD69 (all from BD Biosciences — Pharmingen). CII was isolated from Lewis rat chondrosarcoma by pepsin or lathyritic digestion as described before (48, 49). Chicken egg albumin (OVA) was obtained from Sigma-Aldrich, and PPD was obtained from Statens Serum Institut.

Flow cytometry.

We stained 15 μl of blood or cell suspension for Ncf1 or burst as described before (12, 13). FcR interaction was blocked by incubation in 5% serum before and during the first antibody incubation. We analyzed 1 × 10⁵–5 × 10⁵ cells with a FACSort, and fluorescence was expressed as GeoMeanX (BD). Mouse anti-human Ncf1 cross-reacting with mouse Ncf1 (clone D-10; Santa Cruz Biotechnology Inc.) or an isotype-matched irrelevant control antibody was used. Cell surface –SH groups were detected with Alexa Fluor 488 or 633 coupled to maleimide (Invitrogen) as described previously (12, 22).

T cell activation assays.

Spleens and LNs from naive mice or mice immunized 10 days previously were conferred to cell suspensions. Cells from immunized mice were incubated with lathCII or OVA at different concentrations of antigen or cells. We isolated p-macrophages by injecting 5 ml of ice-cold DMEM into the peritoneal cavity of naive mice; no thioglycollate was used. We depleted p-macrophages from B cells and neutrophils by MACS (Miltenyi); purity was higher than 98%. DCs were grown from bone marrow by stimulation with GM-CSF, as described before (19). DCs were matured with LPS for the last 24 hours. CII was provided for 48 hours, adding ³H-thymidine to allow phagocytosis. APCs were coincubated with HCQ10 hybridoma T cells, recognizing CII in H2-Aq and CII. After 24 hours, supernatant was assayed for IL-2 by sandwich ELISA. For the crisscross experiments (Figure ​(Figure6),6), T cells were isolated from spleens by negative selection by MACS; spleen cells were — after lysing erythrocytes — incubated with biotinylated Ab directed against DCs, macrophages, granulocytes, NK cells, B cells, and CD8. After incubation with streptavidin-magnetic beads (Miltenyi Biotec), cells were separated twice on a magnetic column. The cell suspensions consisted of over 90% CD4⁺ T cells and less than 0.4% of CD11b⁺ cells. The remaining 10% were negative for all markers and seemed to represent erythrocytes on FSC/SSC. Spleen APCs were obtained by depleting for T cells by MACS (anti-CD3/4/8). Twenty-four–hour supernatants were assayed for IL-2; after 72 hours, cells were pulsed with ³H-thymidine for 15-18 hours. Supernatants were then tested for IFN-γ production. For experiments shown in Figure ​Figure7,7, anti-CD3 was used platebound (2 hours at 37°C) with or without soluble anti-CD28 (BD Biosciences — Pharmingen).

ELISAs.

Serum levels of anti-CII IgG were detected by ELISA as described before (4). As a standard, purified anti-CII Ab from immunized DBA/1 mice was used with known concentration. ELISAs to detect TNF-α and IFN-γ were performed in a similar way, using mAb from BD Biosciences — Pharmingen or a kit from Pierce Biotechnology (Endogen; TNF-α). ELISAs to detect IL-4, IL-2, IL-5, IL-10, and IL-17 were developed using streptavidin-europium and enhancement buffer (PerkinElmer). Ab and standards were obtained from BD Biosciences — Pharmingen.

ELISPOT assays.

After prewetting with ethanol, ELISPOT plates were coated with anti–IFN-γ Ab, and spleen or LN cells from immunized mice were divided over the plates in different cell concentrations or at 1 cell concentration of 10⁶ cells, with different concentrations of lathCII. After 24 hours, cells were decanted and IFN-γ was detected with biotinylated anti–IFN-γ, which was detected with streptavidin-labeled alkaline phosphatase. Spots were developed with BCIP/NBT (Sigma-Aldrich). Number of spots was determined with an ImmunoScan ELISPOT reader and analyzed with ImmunoSpot software (Cellular Technology Ltd).

We thank our animal technicians Carlos Palestro and Rebecca Lindqvist; David Greaves, Oxford University, for the promoter construct; the Anna Greta Crafoord Stiftelse för Reumatologisk Forskning, Konung Gustaf V:s 80-års and Wenner Gren Foundation; the EU (MUGEN LSHG-CT-2005-005203, EURAPS LSHM-CT-2005-005223, Neuropromise LSHM-CT-2005-018637) and SSF for grants; and Leendert A. Trouw for carefully reading the manuscript.