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发表于 2009-4-20 09:21 |只看该作者 |倒序浏览 |打印

作者：Ping He1, Zhenyu Zhong1, Kristina Lindholm1, Lilian Berning1, Wendy Lee1, Cynthia Lemere3, Matthias Staufenbiel4, Rena Li2, and Yong Shen1作者单位：1 Haldeman Laboratory of Molecular and Cellular Neurobiology and 2 Roberts Center for Alzheimer's Research, Sun Health Research Institute, Sun City, AZ 85351
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      【关键词】 necrosis
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Introduction

Alzheimer's disease (AD) affects 4.5 million Americans, and this number will continue to grow. By 2050, the number of individuals with AD could range from 11.3 to 16 million (Hebert et al., 2003). The pathogenesis underlying AD remains unclear, and it is controversial whether AD results from a primary abnormality in amyloid precursor protein (APP) or deregulation of the inflammatory system (Weiner and Selkoe, 2002), although these two possibilities are not mutually exclusive. Several lines of evidence implicate abnormal processing of APP, which is cleaved by two enzymes, ?-secretase 1 (BACE1) and -secretase, to generate excessive amyloid ? protein (A?), as a potential cause of AD (Selkoe, 2003; Tanzi and Bertram, 2005). In the past decade, transgenic mice have been generated that overexpress mutant APP and display A?-related lesions (Hsiao et al., 1995). Many of these mouse models exhibit amyloid plaque-predominant aspects of AD (Terry et al., 1987; Tiraboschi et al., 2004), including A? plaque formation, cerebral amyloid angiopathy (CAA), and inflammation, but not pathology.( E9 m/ N" Y! E
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The TNF death receptor belongs to the TNFR superfamily, which includes >20 cell surface receptors. When the TNF type 1 death receptor (TNFR1) binds to its ligand, TNF, the ligand–receptor complex triggers apoptotic pathways by recruiting a TNFR-associated death domain protein and/or a Fas-associated death domain protein/mediator of receptor-induced toxicity, two intracellular adaptor proteins (Boldin et al., 1995). The receptor-induced multimerization of a Fas-associated death domain protein leads to caspase activation, which causes degradation of specific target proteins, ultimately damaging cell integrity (Ashkenazi and Dixit, 1998).# X; H5 w. \7 q" Z

To find out whether TNFR1 could have effect on A? production as well as APP processing, we specifically chose transgenic APP23 mice in our experiments, which express a mutant APP that results in extensive A? plaque formation. Here we show that fewer A? plaques and A?-related lesions develop in Alzheimer's transgenic mice with genetic deletion of TNFR1. Detailed analyses showed decreased A? generation, less neuronal loss, and alleviated A?-related memory deficits. Our data indicates that TNFR1 might be a potential and novel therapeutic target for AD.! `0 m/ J$ L" X' I5 J# v* d& X
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TNFR1 deletion reduces A?-related pathology# N, F+ C4 u( c: V
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APP23 transgenic mice (Sommer and Staufenbiel, 1998), a mouse model for AD with a plaque-predominant type (Terry et al., 1987; Tiraboschi et al., 2004), overproduce A?, A?40, and A?42, and develop significant amyloid deposits by the age of 14 mo. To determine whether genetic inactivation of TNFR1 delays or diminishes A? plaque formation, we crossed APP23 mice with mice lacking the TNFR1 gene (TNFR1–/–; Peschon et al., 1998) to generate APP23/TNFR1–/– mice. To evaluate A? pathology in the brains, we first used Congo red staining to see if reduced protein aggregation could be observed in the brains of APP23/TNFR1–/– mice. Congo red has been shown to be affinitive for binding to fibril proteins enriched in ?-sheet conformation, and it is commonly used as a histological dye for amyloid detection (Frid et al., 2006). Results showed much less Congo red staining in APP23/TNFR1–/– mice (Fig. 1 A), indicating that protein aggregation was alleviated in APP23/TNFR1–/– mice." S6 @6 f8 Q% p* a

Figure 1. A? deposition is significantly reduced in APP23/TNFR1–/– mice. (A) Congo red showed fewer congophilic deposits in the brains of APP23/TNFR1–/– mice at both 12 and 24 mo of age. (B) 6E10-immunostained sections of the entorhinal cortex. (C) Stereological analyses of 6E10-immunostained sections revealed fewer immunoreactive plaques in the entorhinal cortex of APP23/TNFR1–/– mice. (D) 6E10-immunostained sections of the hippocampus. (E) Stereological analyses of 6E10-immunostained sections revealed fewer immunoreactive plaques in the hippocampus of APP23/TNFR1–/– mice (*, P 20 μm) were found in the entorhinal cortex of APP23/TNFR1–/– mice. (G) Fewer large plaques (>20 μm) were found in the hippocampus of APP23/TNFR1–/– mice. Error bars represent SD. Bars, 50 μm.$ T% ~, j5 o0 G: E

To further confirm that the aggregated protein we found was aggregated A? peptide, we next examined the brain section with anti-A? antibody 6E10 (Vassar et al., 1999; Van Dooren et al. 2006). At 12 mo of age, APP23 mice displayed numerous A? plaques throughout the entorhinal cortex and hippocampus, consistent with a previous paper (Sommer and Staufenbiel, 1998). In APP23/TNFR1–/– mice, however, we found only minor A? plaques in the entorhinal cortex (Fig. 1, B and C) and the hippocampus (Fig. 1, D and E). At 24 mo of age, APP23/TNFR1–/– mice also displayed reduced plaques (Fig. 1, B and D). The number of plaques was reduced by 73 and 80% in the entorhinal cortex (Fig. 1 C) and hippocampus (Fig. 1 E) in APP23/TNFR1–/– mice at 12 mo of age, indicating that A? pathology in APP23/TNFR1–/– indeed alleviated plaque formation compared with age-matched APP23 mice.) i/ @: g8 t& C3 y3 F' h
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The size of A? plaques also indicates the severity of A? pathology (Zhou et al., 2005). We used morphometric analyses on the brain sections immunostained with A? antibody 6E10. Results showed that both large (>20 μm diameter)- and medium (10–20 μm diameter)-sized A? plaques in the entorhinal cortex (Fig. 1 F) and hippocampus (Fig. 1 G) were significantly reduced in APP23/TNFR1–/– mice at 12 and 24 mo of age, indicating that in APP23/TNFR1–/– mice, A? pathology was alleviated not only by reducing the overall A? plaque number, but also by decreasing plaque size.% ^; _/ T9 _/ `

TNFR1 deletion reduces CAA  o# z$ @7 C! c; }9 J) i

CAA has been reported to have both positive and negative correlations with AD pathology (Cohen et al., 1997; Thal et al., 2003; Tian et al., 2003). It has been shown that CAA in APP23 transgenic mice is strikingly similar to that of human CAA (Calhoun et al., 1999). To find out whether genetic deletion of TNFR1 can relieve CAA in APP23 mice, the deposition of A? in the vascular wall was examined by double immunostaining with antibodies against ?-smooth muscle actin (a vascular smooth muscle marker; Skalli et al., 1986) or von Willebrand factor (vWF; an endothelial cell marker; Shyu et al., 2006) and anti-A?40 antibody. We found that at 24 mo of age, APP23 mice display CAA predominant in cortical, hippocampal, and thalamic vessels; A?40 formed a continuous ring-like shape within the vessel wall (Fig. 2, A and B), consistent with Calhoun et al. (1999). However, there were very few A?40 deposits within the vessels of APP23/TNFR1–/– (Fig. 2, C and D). Deposition of A? on the vascular wall could not only increase the vulnerability of cerebral vessels but also increase the possibility of intracerebral hemorrhage (Vinters, 1987; Itoh et al., 1993; Winkler et al., 2001; Atwood et al., 2003). Our results showed little CAA progression in the brains of APP23/TNFR1–/– mice, suggesting that deletion of TNFR1 could reduce the risk of CAA.
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Figure 2. Cerebral vascular amyloid deposits were reduced in APP23/TNFR1–/– mice. (A) 6E10 immunostaining showed that microvascular A? deposits were reduced in the frontal cortex of APP23/TNFR1–/– mice. (B) Vascular A? deposits were reduced in the thalamus of APP23/TNFR1–/– mice. (C) Double labeling of -smooth muscle actin (-SM actin; red) and A?40 (green) showed fewer A?40 deposits on microvascular walls of 24-mo-old APP23/TNFR1–/– mice than in age-matched APP23 mice (arrow points to absence of A? deposits on one smaller vascular wall). (D) Double labeling of 6E10 and vWF antibody showed fewer A? deposits on the vascular walls of 24-mo-old APP23/TNFR1–/– mice (arrow points to an A? plaque that appears to be outside of the vascular wall in the cortex of APP23/TNFR1–/– mice). Bars: (A and B) 50 μm; (C and D) 5 μm.1 `1 f  y/ n" p9 c6 F5 N
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TNFR1 deletion reduces microglia activation

Microglia activation is also a hallmark of A? pathology progression (Yan et al., 2003 ;Wilcock et al., 2004; Simard et al., 2006). CD11b and CD45 are two well-characterized markers for microglia activation in the brains (Yan et al., 2003; Wilcock et al., 2004; Simard et al., 2006).To examine whether deletion of TNFR1 could alleviate the massive microglia activation of APP23 mice, we studied the microglia activation in APP23 and APP23/TNFR1–/– mice. Consistent with a previous paper (Wilcock et al., 2003), APP23 mice showed strong immunoreactivity with antibodies against CD11b (Mac-1) and CD45 in the entorhinal cortex (Fig. 3 A) and hippocampus (Fig. 3 B), indicating that a massive amount of microglia had been activated along with the appearance of A? pathology. In contrast, APP23/TNFR1–/– mice showed significantly less CD11b and CD45 immunoreactivity in the entorhinal cortex (Fig. 3 A) and hippocampus (Fig. 3 B), indicating that genetic deletion of TNFR1 alleviated massive microglia activation in APP23 mice.

Figure 3. Microglia activation is reduced in the brains of APP23/TNFR1–/– mice. (A) The sections were immunostained with CD11b, an activated microglia marker, in the entorhinal cortex. (B) The sections were immunostained with CD11b in the hippocampus. Bars, 50 μm." Y, C& e* j1 [

TNFR1 deletion reduces A? production

Because we found reduced A? pathology in APP23/TNFR1–/– mice, our next question was whether genetic inactivation of TNFR1 reduces A? pathology by affecting A? generation. The A? level was analyzed by immunoprecipitation followed by Western blotting (n = 3 for each group). Fig. 4 A shows a representative urea Western blot (Wiltfang et al., 1997) comparing the 4-kD A? species (n = 3 for each group). Both A?40 and A?42 can be detected, and A?42 migrated ahead of A?40, consistent with a previous paper (Wiltfang et al., 1997). Compared with APP23 mice, APP23/TNFR1–/– mice showed a significant reduction in both A?40 and A?42 levels (Fig. 4 A). We further measured total A?, A?40, and A?42 levels by sandwich ELISAs (n = 10 for each group). The results bolstered our Western blot findings and confirmed that APP23/TNFR1–/– mice have much less total A?, A?40, and A?42 (Fig. 4, B–D). Quantitatively, total A? decreased by 69% (37.39 ± 12.71 ng/mg) and 30% (463.87 ± 189.83 ng/mg) in 12- and 24-mo-old APP23/TNFR1–/– mice, respectively, compared with total A? in APP23 mice (12 mo old: 120.80 ± 39.74 ng/mg; 24 mo old: 693.40 ± 270.27 ng/mg; Fig. 4 B). Both A?40 and A?42 were reduced in APP23/TNFR1–/– mice. However, the most significant difference is at 12 mo of age, when A?40 decreased by 80% in APP23/TNFR1–/– mice (20.45 ± 4.7 ng/mg) compared with APP23 mice (103.87 ± 21.81 ng/mg; Fig. 4 C), and A?42decreased by 70% in APP23/TNFR1–/– mice (4.12 ± 1.2 ng/mg) compared to APP23 mice (15.78 ± 4.7 ng/mg; Fig. 4 D). These results indicated that reduction in A?40 and A?42 levels could account for the alleviated A? pathology in APP23/TNFR1–/– mice.
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Figure 4. Deletion of TNFR1 reduces A? production. (A) Western blot showed reduced A?40 and A?42 in APP23/TNFR1–/– mice at both 12 and 24 mo of age. (B) Total A? ELISA was calculated as nanogram per milligram of protein. (C) A?40 ELISA was calculated as nanogram per milligram of protein. (D) A?42 ELISA was calculated as picogram per milligram of protein (*, P
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One of the mechanisms that could influence A? production is through altering APP holoprotein levels. We next analyzed by Western blot to see if deletion of TNFR1 affects APP protein levels (n = 3 for each group). In contrast to the reduction in A? levels, Western blotting did not reveal any differences in full-length APP levels between APP23/TNFR1–/– and APP23 mice (Fig. 4 E), indicating that the decrease in A? levels was not caused by altering APP protein expression in APP23/TNFR1–/– mice." H, L% o8 Y) _% H+ H2 l6 G3 Z

TNFR1 deletion alters BACE1 activity and level

To examine whether the reduced amyloidosis in APP23/TNFR1–/– mice was caused by a reduction in abnormal APP metabolism, we examined the activity and expression levels of one key enzyme in APP processing, BACE1.
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We first used an MCA-labeled BACE1 substrate (Yang et al., 2003; Li et al., 2004a) to examine BACE1 activity and found that BACE1 activity was significantly decreased in APP23/TNFR1–/– mice (Fig. 5 A). To find out whether the decreased BACE1 activity was due to a decrease in BACE1 levels, we measured BACE1 levels by sandwich ELISA (Yang et al., 2003) and Western blot (n = 3 for each group). We found that BACE1 levels in APP23/TNFR1–/– mice were indeed reduced in both Western blot and ELISA results (Fig. 5, B and C), indicating that reduced BACE1 activity in APP23/TNFR1–/– mice was caused by a reduction in the protein level. To further investigate whether reduced BACE1 protein level is caused by reduced BACE1 mRNA transcription, we performed RT-PCR to measure BACE1 mRNA levels and found that BACE1 mRNA was also decreased in APP23/TNFR1–/– mice (Fig. 5 D), indicating that the genetic deletion of TNFR1 reduced BACE1 mRNA levels and caused BACE1 activity to be down-regulated in APP23/TNFR1–/– mice.

Figure 5. Deletion of TNFR1 reduced BACE1 protein levels and activity. (A) BACE1 activity assay showed reduced BACE1 activity in APP23/TNFR1–/– mice at 12 and 24 mo, compared with APP23 mice. The activity was normalized to the input protein amount and indicated as an arbitrary unit (*, P
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TNF regulates BACE1 transcription through the TNFR1–nuclear factor B (NF-B) pathway% O8 L6 G! d& R8 L
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Our RT-PCR results showed that BACE1 mRNA levels decreased in APP23/TNFR1–/– mice; the next question was what signal transduction pathway leads to the decreased BACE1 mRNA level.

To clarify how deletion of TNFR1 affects BACE1, we transfected 293 cells with a pB1P-A vector containing a BACE1 promoter (–1941 to  292) that was upstream of a luciferase reporter gene (Christensen et al., 2004; Sambamurti et al., 2004), and then treated these cells with different concentrations of TNF. We found that BACE1 promoter activity increased in a concentration-dependent manner (Fig. 6 A). Blocking the interaction of TNF with the extracellular domain fragment of TNFR1 inhibited such elevation in BACE1 promoter activity (Fig. 6 A), indicating that TNF activates BACE1 promoter through TNFR1.! L0 }) c+ T+ S% X1 H; v* b8 j3 w

Figure 6. TNFR1 regulates BACE1 promoter activity through NF-B. (A) TNF induces BACE1 promoter activity. (B) NF-B inhibits TNF-induced BACE1 promoter activity. Error bars represent SD.0 M2 q$ ]" A6 O1 x1 c
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NF-B is one of the major mediators of TNF-activated TNFR1 signaling (Hsu et al., 1995; Yang et al., 2002). A recent finding that multiple NF-B binding sites are located in the vicinity of BACE1 promoter (Sambamurti et al., 2004) suggests that NF-B may play an important role in regulating BACE1 transcription. To determine whether TNFR1 activates the BACE1 promoter through this pathway, we used the potent NF-B activation inhibitor 6-amino-4(4-phenoxyphenylethylamino) quinazoline (Tobe et al., 2003) to block NF-B signaling in TNF- treated 293 cells transfected with a BACE1 promoter luciferase reporter vector. Treating a pB1P-A transfected cell with an NF-B inhibitor significantly reduced TNF-induced BACE1 promoter activity (Fig. 6 B). A high concentration of NF-B inhibitor inhibited not only TNF-induced BACE1 promoter activity but also basal promoter activity (Fig. 6 B), indicating that NF-B may play a central role in regulating BACE1 transcription. Thus, the TNF-mediated activation of NF-B through TNFR1 represents a key part of this regulatory pathway.0 k) [6 k& [& L# D9 \* G4 L

These findings indicate that one mechanism underlying the regulation of BACE1 transcription may be through TNFR1-mediated activation of NF-B. We found significantly lower A? as well as BACE1 levels in APP23/TNFR1–/– in older specimens (12 and 24 mo). One possible explanation is that when A? deposits are lower (at both time points), there is less A? to extract, therefore lower A? levels might not be caused by the reduced BACE1 level. To examine whether the reduced A? level is caused by the reduced BACE1 level, we measured A? and BACE1 levels in APP23/TNFR1–/– mice at 6 mo of age, before A? pathology can be observed. If TNFR1 affects the BACE1 level, it should also reduce the BACE1 level at this age. We first found that total A? in APP23/TNFR1–/– mice was much lower than in APP23 mice (Fig. 7 A). Both A?40 and A?42 levels in APP23/TNFR1–/– mice were also reduced. A Western blot showed a reduction of the BACE1 protein level in APP23/TNFR1–/– mice (Fig. 7 B). BACE1 RT-PCR showed a similar result to that of 12-mo-old mice; the BACE1 mRNA level was significantly lower in APP23/TNFR1–/– mice than in APP23 mice (Fig. 7 C). Together, these findings indicate that TNFR1 indeed regulates the BACE1 mRNA level, and that A? reduction in APP23 mice after genetic deletion of TNFR1 is caused by decreased BACE1 levels.5 K! L$ b9 H* ^- i1 s$ f

Figure 7. A? and BACE1 levels are reduced in APP23/TNFR1–/– mice as early as 6 mo of age. (A) A?40 and A?42 levels of APP23 and APP23/TNFR1–/– mice at 6 mo of age. (B) Western blots showed that BACE1 in APP23/TNFR1–/– mice is much lower than that in PP23 mice at 6 mo of age. (C) RT-PCR showed that BACE1 mRNA in APP23/TNFR1–/– mice is significantly lower compared with APP23 mice at 6 mo of age. Error bars represent SD.

TNFR1 deletion has little effect on A? clearance enzymes insulin degradation enzyme (IDE) and neprilysin (NEP)7 R! `( B; e+ Y! H4 Y; B* b
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A? reduction could also be caused by an increase in A? degradation/clearance activity, which is not relevant to A? production. To determine whether deletion of TNFR1 reduces A? deposition by affecting enzymes involved in A? degradation, we assessed the protein levels of IDE and NEP, two enzymes that play an important role in A? degradation and clearance (Farris et al., 2003). Western blot analyses did not show significant differences in either IDE or NEP levels between APP23/TNFR1–/– and APP23 mice (Fig. 8 A), suggesting that deletion of TNFR1 did not interfere with IDE and NEP expression. To find out whether deletion of TNFR1 could have an effect on IDE or NEP activity, we further compared both IDE and NEP activity between APP23 and APP23/TNFR1–/– mice. Again, no significant difference was observed (Fig. 8, B and C). Therefore, IDE and NEP were not responsible for the reduction of the A? level associated with the TNFR1 deletion.* N1 `- t  W, p2 p. ]0 _4 [7 `+ w- f' K
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Figure 8. Deletion of TNFR1 has no effect on IDE or NEP. (A) Western blots showing the density of IDE and NEP in brain lysates of wild-type, APP23/TNFR1–/–,and APP23 mice at 12 and 24 mo of age. (B) No significant changes were observed in IDE activity between APP23 and APP23/TNFR1–/– mice. (C) No significant differences in NEP activity between APP23 and APP23/TNFR1–/– mice were found. Error bars represent SD.

TNFR1 deletion ameliorates neuron loss
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We recently reported that TNFR1 plays a critical role in A?-induced neuronal death (Li et al., 2004b). To determine whether the deletion of TNFR1 protects neurons, we compared neuronal loss in wild-type, APP23/TNFR1–/–, and APP23 mice. Compared with wild-type mice, APP23 mice show a 30% reduction in NeuN-positive cells in the entorhinal cortex, whereas APP23/TNFR1–/– mice show no significant reduction at 24 mo of age (Fig. 9, A and C). Results were similar in the hippocampus, where APP23 mice had 15% fewer NeuN-positive cells in the CA1 area of the hippocampus (Fig. 9 B, D; Calhoun et al., 1998), whereas little neuronal loss was seen in APP23/TNFR1–/– mice at 24 mo of age (Fig. 9, B and D). We found similar results using Nissl-stained brain sections (not depicted).

Figure 9. Deletion of TNFR1 in APP23 mice reduces neuron loss. (A) Fewer NeuN-positive neurons were present in the entorhinal cortex of APP23 mice at the age of 24 mo. (B) NeuN immunostaining demonstrated little neuronal loss in the CA1 field in APP23/TNFR1–/– mice. (C) Statistical analyses show that APP23 mice had significantly fewer neurons in the entorhinal cortex at 24 mo of age (*, P
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TNFR1 deletion lessens memory deficits typical of APP23 mice# C/ i. p! W. f6 k3 i1 \

To examine the behavioral significance of TNFR1 deletion, we tested wild-type, APP23, APP23/TNFR1–/–, and TNFR1–/– mice with a hole-board memory test, which is a behavioral task widely used to assess exploratory learning and memory (Garcia, 1987; Thifault et al., 2002). The majority of APP23 mice showed significant deficits in the spatial component of the test. However, exploratory learning and memory retention (percentage of correct pokes) of APP23/TNFR1–/– mice was not significantly different from that of wild-type or TNFR1–/– mice (Fig. 10 A). This suggests that deletion of TNFR1, which could lead to a reduction of A? levels as well as neuronal protection, might have an effect on improving spatial learning performance in APP23/TNFR1–/– mice (Fig. 10 A). The correlation between A? reduction/neuronal protection and improved learning and memory behaviors remained strong when the percentages of correct pokes were averaged over all hidden hole-board trials (Fig. 10 A). Specifically, we found that 6-mo-old APP23 mice made more errors than did age-matched wild-type mice across 3 d of testing (group effect, F1,15 = 22.198, P 3 R3 ~0 y' c8 U5 |
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Figure 10. Deletion of TNFR1 improves learning and memory. (A) The percentage correct of finding a cheese reward hidden in one hole of the hole-board task (Brosnan-Watters and Wozniak, 1997). Data were calculated as percentages (mean ± SEM; *, P # m) n8 S! i* h4 o- w) s  a5 J
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The object recognition task is based on the spontaneous exploration of novel and familiar objects. Mice will spend more time exploring a novel object than a familiar one (Pittenger et al., 2002; Bourtchouladze et al., 2003; Wang et al., 2004). We further examined whether deletion of TNFR1 could rescue object recognition deficits in APP23 mice. Object recognition performance was much better in APP23/TNFR1–/– mice than in APP23 mice, as the recognition indexes differed significantly between these groups (group effect, F3,31 = 24.947, P
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Discussion
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TNFR is a family of TNF receptors, TNFR1 and TNFR2 (Tartaglia et al., 1993), both of which bind soluble A?40 (Li et al., 2004b). Overexpression of TNFR1 promotes A?-induced neuronal death (Li et al., 2004b). It has been reported that a higher inflammatory response was observed in MCI and AD patients (Cagnin et al., 2001; Tarkowski et al., 2003 ;Galimberti et al., 2006), and inflammatory cytokines and free radicals can up-regulate BACE1 expression (Tamagno et al., 2002; Hong et al., 2003; Pak et al., 2005; Tamagno et al., 2005; Sastre et al., 2006). TNF is one of the up-regulated inflammation factors in APP transgenic mice (Patel et al., 2005). Here we found that TNFR1 could directly regulate BACE1 transcription through NF-B, which is one of the major mediators of TNF-activated TNFR1 signaling (Hsu et al., 1995; Yang et al., 2002). Recent findings showed multiple NF-B binding sites located in the vicinity of BACE1 promoter (Sambamurti et al., 2004), suggesting that NF-B may play an important role in regulating BACE1 transcription. This is confirmed by our results that the NF-B inhibitor inhibits BACE1 promoter activity.

At 24 mo of age, we found significant neuronal loss in APP23 mice. However, Irizarry et al. (1997) did not observe neuronal loss in 16-mo-old APP transgenic mice (Tg2576) expressing the APPK670N/M671L mutation, the same mutation harbored by APP23 mice. This might be because the APP transgene is controlled by different promoters in APP23 and Tg2576 mice (Irizarry et al., 1997; Sturchler-Pierrat et al., 1997). TNFR1 deficiency ameliorates neuron loss in APP23 mice, consistent with our previous findings that TNFR1 overexpression increases the vulnerability of cultured hippocampal neurons to A?-induced death and promotes neuronal degeneration (Li et al., 2004b). We also noticed that TNF plays different roles in neuronal death and survival via its distinct receptors, TNFR1 and TNFR2. Neuron loss in APP23 mice caused by "endogenous" A? may be conducted through different signal transduction pathways. Moreover, Barger et al. (1995) showed that TNF can protect neurons derived from fetal brains against A? toxicity. Our unpublished data show that TNFR1 is expressed at a low level, whereas TNFR2 is expressed at a high level in fetal neurons. This may explain why TNF is trophic in fetal neurons. Interestingly, Bruce et al. (1996) discovered that neurons from mice with a deficiency of both TNFR1 and TNFR2 are more sensitive to excitotoxic injury. This result is interesting because the finding suggests that there is a balance between TNFR1 and TNFR2 expression levels in neurons, and TNFR2 seems to be more critical and more sensitive to neurons.

Our behavioral analyses revealed that inactivation of TNFR1 rescued hippocampal-dependent learning and memory deficits displayed by young APP23 mice (Van Dam et al., 2003). A previous study reported that disruption of the BACE1 gene or PS1 in APP transgenic mice rescues memory deficits measured by social recognition and spatial alternation tasks (Saura et al., 2005). This is consistent with our findings in APP23/TNFR1–/– mice, presumably because TNFR1 depletion decreases A? production and deposition, thereby reducing A?-related memory deficits. The relatively normal performance of hippocampal-dependent memory tasks by APP23/TNFR1–/– mice is age related. At 6 mo of age, APP23/TNFR1–/– mice already performed hippocampal-dependent memory tasks better than APP23 mice. Furthermore, TNFR1 knockout mice exhibited normal synaptic transmission and plasticity in the Schaffer collateral pathway (unpublished data). Our results allow us to determine whether treating APP23 mice with anti-TNFR1 antibody or inhibitors of the TNFR1 signal transduction pathway could reduce BACE1 and cerebral A?.+ u. e+ q$ n4 A0 f
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Materials and methods9 V4 D- U" k! V2 U: g

Generation of APP transgenic AD mice with deletion of TNFR1
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TNFR1 knockout mice (TNFR1–/–) were constructed on a C57BL/6 background as previously described (Peschon et al., 1998). APP23 transgenic mice were provided by Novartis Institute for Biomedical Research; these mice express mutant human ?APP (Swedish double mutation, KM670/671NL) under the control of a brain- and neuron-specific murine Thy-1 promoter element. APP23 transgenic mice develop senile plaques in the cerebral cortex and hippocampus and show neuronal loss at 12–18 mo of age; this pathology is most evident in area CA1 of the hippocampus (Sommer and Staufenbiel, 1998). APP23 mice were also constructed on a C57BL/6 background.* `  m' n7 Q4 |' p0 y& F% @/ O

APP23 and TNFR1–/– mice were crossed and their progeny were genotyped. An APP23/TNFR1 /– mouse was backcrossed with TNFR1–/– mice to produce APP23/TNFR1–/– mice. To maintain the heterozygous APP transgene in our mice, we crossed APP23 mice with wild-type C57BL/6 mice. For APP23/TNFR1–/– mice, we crossed APP23/TNFR1–/– with TNFR1–/– mice for three to five generations. Therefore, both APP23 and APP23/TNFR1–/– mice were APP23 /–. We used APP23/TNFR1–/– mice of the F3–F5 generation in our experiments.
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Mice homozygous for the TNFR1 targeted mutation (formerly TNFR1, p55 deficient) show defects in resistance to intracellular pathogens and are resistant to the lethal effects of lipopolysaccharide administration in conjunction with D-galactosamine. Pulmonary inflammatory responses are diminished in p55-deficient mice. There are also defects in splenic architecture, formation of germinal centers, and liver regeneration. TNFR1- deficient mice display increased susceptibility to atherosclerosis when maintained on a high-fat diet (Peschon et al., 1998). No observations regarding any syndromes of the central nervous system have been made.6 k1 n; v( X  Q

ELISA
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APP23, APP23/TNFR1–/–, and wild-type mice (n = 10 per group) were killed at 12 and 24 mo of age, and one hemisphere of the brain was homogenized in homogenization buffer (250 mM sucrose, 20 mM Tris-HCl, pH 7.4, 1 mM EDTA, and 1 mM EGTA). An aliquot of the homogenate was dissolved in formic acid and neutralized with a neutralization buffer (1 mM Tris and 0.5 M Na2HPO4). Protein concentration was measured by protein assay (Bio-Rad Laboratories). For total A? ELISA, the capture antibody was monoclonal anti-A? antibody 4G8 (Chemicon), and the detection antibody was biotinylated monoclonal antibody anti-A? 6E10 (AbD Serotec). A?40 and A?42 were measured with an A?40 and A?42 ELISA kit (Biosource International). The ELISA system has been extensively tested and no cross-reactivity between A?40 and A?42 was observed. Data are presented as means ± SD of four experiments.  _1 ]* a: {, F! p1 Y
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BACE1 protein levels were measured by ELISA as described previously (Yang et al., 2003). The capture antibody was anti-BACE1 polyclonal antibody P1 (Yang et al., 2003) and the detection antibody was biotinylated anti-BACE1 polyclonal antibody P2 (Yang et al., 2003). TMB substrate was used to visualize the reaction product, which was read at OD450 with a microplate reader (Sigma-Aldrich). BACE1 protein (Amgen) was used as a standard. Data are presented as means ± SD of four experiments.
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Western blot! g9 K8 i+ l  o" V; w1 x5 m- I+ K

Aliquots of brain homogenates from APP23, APP23/TNFR1–/–, and wild-type mice were further lysed with 1x RIPA buffer, and 50–150 μg of total protein was subjected to SDS-PAGE (8–12% acrylamide). Separated proteins were then transferred onto polyvinylidene fluoride membranes. The blots were probed with the following antibodies: anti-BACE1 monoclonal antibody (R&D Systems), anti-A? (1–17) monoclonal antibody (clone 6E10, 1:2,000; Chemicon), anti-IDE polyclonal antibody (Oncogene Research Products), anti-NEP polyclonal antibody (Chemicon), and anti– ? actin antibody (Sigma-Aldrich).9 b; Q% W+ ]/ _. k7 y8 P6 W

Western blotting for A? was performed as described previously (Wiltfang et al., 1997). To detect minute levels of A?, formic acid–dissolved brain tissue was immunoprecipitated with anti-A? polyclonal antibody (Zymed Laboratories) and subjected to SDS-PAGE using 10% acrylamide gels containing 8 M urea. Separated proteins were transferred onto polyvinylidene fluoride membranes. A?40 and A?42 were detected with monoclonal anti-A? antibody 6E10. Synthetic A?40 and A?42 (Biosource International) were used as standards.1 C9 L6 }6 S) j9 Z+ k/ e7 j- I

BACE1, IDE, and NEP activity
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An aliquot of brain homogenates from APP23, APP23/TNFR1–/–, and wild-type mice was further lysed with a lysis buffer (10 mM Tris-HCl, pH 7.4, 150 mM NaCl, 1 mM EDTA, 1 mM EGTA, 1 mM Na3VO4, 10% glycerol, and 0.5% Triton X-100). BACE1 enzymatic activity assays were performed by using synthetic peptide substrates containing BACE1 cleavage site (MCA-Glu-Val-Lys-Met-Asp-Ala-Glu-Phe--OH; Biosource International). BACE substrate was dissolved in DMSO and mixed with a 50-mM Hac and 100-mM NaCl, pH 4.1, reaction buffer. An equal amount of protein was mixed with 100 μl of substrate, and fluorescence intensity was measured with a microplate reader (BioTek) at an excitation wavelength of 320 nm and an emission wavelength of 390 nm.

IDE enzyme activity was measured as described previously (Song et al., 2003). In brief, brains were homogenized in 50 mM potassium phosphate buffer, pH 7.3, containing 200 μm PMSF and a proteinase inhibitor mix (Sigma-Aldrich). Samples were centrifuged and the supernatant fraction was used for IDE activity measurement. The hydrolysis of fluorogenic substrate peptides (2 μm Abz-GGFLRKHGQED-Dnp as substrate in 20 mM potassium phosphate buffer, pH 7.3) was measured by following an increase in fluorescence (excitation at 318 nm and emission at 419 nm) that occurred upon peptide bond cleavage. The max velocity of IDE activity was calculated by the first 20 min and indicated as fluorescence unit/min microgram protein.+ W0 f6 Z% C; r) F$ y+ Y+ s

For the in vitro NEP activity assay, mouse brains were homogenized in 100 mM MES buffer (pH 6.5) with proteinase inhibitors (Sigma-Aldrich). Homogenate was centrifuged at 20,000 g for 45 min to separate the membrane fraction and the supernatant was removed. The membrane pellet was resuspended in MES buffer and directly used in NEP activity assay as previously described (Li and Hersh, 1995).

RT-PCR; L) a! h- l! K& g
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To compare BACE1 expression levels, we used the following primers for RT-PCR: mouse BACE1 forward primer, 5'-AGACGCTACACATCCTGGTG-3', and backward primer, 5'-CCTGGGTGTAGGGCACATAC-3'. The amplified BACE1 fragment was 146 bp. Mouse s18 was used as a loading control: forward primer, 5'-CAGAAGGACGTGAAGGATGG-3', and backward primer, 5'-CAGTGGTCTTGGTGTGCTGA-3'. The amplified mouse s18 fragment was 159 bp. Total RNA was extracted from the brains of 12-mo-old APP23 and APP23/TNFR1–/– mice (n = 5) using an RNA mini column kit (Invitrogen). RT-PCR was performed using a One- Step RT-PCR kit (Invitrogen) and the following PCR cycles: 50°C for 30 min, 94°C for 2 min, followed by 25 cycles at 94°C for 15 s, 49°C for 30 s, and 68°C for 1 min.

Cell transfection and luciferase assay1 F3 A' B/ T; j2 Q: c" U# F/ S2 [
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We transfected 293 cells with pB1P-A vector containing a BACE1 promoter (–1941 to  292) upstream from a luciferase reporter gene (Christensen et al., 2004) using lipofectamine (Invitrogen). After transfection, cells were treated with different concentrations of TNF (R&D Systems), extracellular domain of TNFR1 (R&D Systems), or NF-B inhibitor 6-amino-4(4-phenoxyphenylethylamino) quinazoline (Calbiochem; Tobe et al., 2003). Cells were collected 12 h after treatment, and a luciferase assay (Promega) was performed, according to the manufacturer's instructions. Luminescence intensity was measured with a microplate reader, normalized according to protein amount, and plotted as relative luminescence units per milligram of protein.

Immunohistochemistry and immunofluorescence

Immunohistochemistry was performed as previously described (Matsuoka et al., 2001). In brief, paraformaldehyde-fixed brains were quickly frozen, and then sectioned at 30 μm. Sections were incubated with either anti-A? (6E10 clone or 4G8 clone, 1:1,000; Chemicon), anti-NeuN (MAB377, 1:400; Chemicon), anti-CD11b (MCA711, 1:500; AbD Serotec) and CD45 (MCA1388, 1:500; AbD Serotec), anti--smooth muscle actin (-SM actin, A2547, 1:400; Sigma-Aldrich), or anti-vWF (AB7536, 1:200; Chemicon). Secondary antibodies were applied with horse anti–mouse (for 6E10, NeuN detection, 1:1,000) and goat anti–rat (for CD45 or CD11b, 1:1,000) followed by a DAB substrate (Vector Laboratories). For immunofluorescence, fluorescent-labeling 488 (green) or 594 (red) secondary antibodies against rabbit IgG or mouse IgG were used (1:1,000; Invitrogen). A microscope (DMLS; Leica) with a 10x N PLAN and 20x and 40x PL FLUOTAR was used. Digital images were captured and processed by digital camera (Optronics) and MagnaFire software (version 2.1C; Optronics).

Quantitation of immunoreactive structures, ~3 ]# ?: [2 l, e
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30-μm serial sagittal sections through the entire rostrocaudal extent of the hippocampus were cut on a cryostat. Every 10th section was immunostained with anti-NeuN antibody. On all sections containing the hippocampus, we delineated the pyramidal cell layer CA1. The total number of neurons were obtained using unbiased stereology (Casas et al., 2004; Schmitz et al., 2004) and a microscope equipped with a digital camera (DEI-470; Optronics). For each section, we delineated a 400-μm2 area in CA1 and in the entorhinal cortex and counted all NeuN-immunoreactive cells within that 400-μm2 box. The mean sum of neurons was counted per animal (n = 10). We used the same method to count A?-immunoreactive plaques (stained with 6E10) in the hippocampus and entorhinal cortex in a double blind test. We also measured the diameter of each counted plaque. Differences between groups were tested with Image-pro Plus Analysis (Media Cybernetics).+ B. B7 t3 }7 a+ d+ ~
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Hole-board memory task: b8 \  X) @& Z4 `# j3 Q- i

As previously reported (Dodart et al., 2002), this task measured a mouse's ability to remember which one out of four equidistant holes was baited with food. Two photobeam apparatuses were used with a hole board for assessing directed exploration in mice for behavioral tests. A tested mouse (n = 10 for each group) was placed in the center of the hole-board and the number of nose pokes was automatically registered for 5 min. After 20 min, each animal was placed in a corner of the hole board and allowed to freely explore the apparatus for 5 min. The number of head dips, time spent head-dipping, and the number of rearings were recorded. A comprehensive cognitive performance was determined by calculating the mean number of correct pokes per trial that mouse made each day. Cognition was expressed as the percentage of correct pokes. The measurements in the hole-board test were analyzed by unpaired t test. In all cases the significance level was considered to be P   v6 _9 `9 y! `' r
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Object recognition task! m4 j" }# T0 f* F4 u
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The day before training, an individual mouse (n = 10 for each group) was placed into a training apparatus (a box the same size as described for the hole-board test) and allowed to habituate to the environment for 15 min. Training was initiated 24 h after habituation. A mouse was placed back into the training box containing two identical objects A and B (die or marble) and allowed to explore these objects. Among experiments, training times varied from 3.5 to 20 min. For each experiment, the same set of animals was used repeatedly with different sets of objects for each repetition. Five repetitions were performed on each set of mice. Each mouse was trained and tested no more than once per week, with a 1-wk interval between testing. Moreover, each experimental condition was replicated independently four times. In each experiment, the experimenter was blinded to the subjects during training and testing. To test memory retention, mice were observed for 10 min, 6 h, and 24 h after training. Mice were presented with two objects, one that was used during training, and thus was "familiar," and one that was novel. The test objects were divided into 10 sets of "training" plus "testing" objects, and a new set of objects was used for each training session. A recognition index was calculated for each mouse, expressed as the ratio (100TB)x(TA TB), where TA and TB are the time spent during the second trial on subject A and subject B, respectively. To ensure that the discrimination targets did not differ in odor, the apparatus and the objects were thoroughly cleaned with 90% ethanol, dried, and ventilated for a few minutes after each experiment.5 A# g# P+ O5 O/ R) G# F

Statistical analyses
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In general, analysis of variance models (ANOVA) were used to analyze behavioral data. Typically, the statistical models included two between-subjects variables, the genotype of mice (APP23 vs. APP23/TNFR1–/–) and age, and one within-subjects variable, such as blocks of trials. When ANOVAs with repeated measures were conducted, the Huynh-Feldt adjustment of levels was used for all within-subjects effects containing more than two levels to protect against violations of the sphericity/compound symmetry assumptions underlying this ANOVA model.- z, G& c, Y/ y3 Q3 v, b
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Acknowledgments/ m! [5 J/ _# i3 t

This work was, in part, supported by the Alzheimer's Association, the Arizona Biomedical Research Consortium (ADRC0020), and the National Institute on Aging (AG025888).
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