Mutations and polymorphisms in the gene encoding factor H (CFH) have been associated with atypical haemolytic uraemic syndrome, dense deposit disease and age-related macular degeneration. The disease-predisposing CFH variants show a differential association with pathology that has been very useful to unravel critical events in the pathogenesis of one or other disease. In contrast, the factor H (fH)-Ile62 polymorphism confers strong protection to all three diseases. Using ELISA-based methods and surface plasmon resonance analyses, we show here that the protective fH-Ile62 variant binds more efficiently to C3b than fH-Val62 and competes better with factor B in proconvertase formation. Functional analyses demonstrate an increased cofactor activity for fH-Ile62 in the factor I-mediated cleavage of fluid phase and surface-bound C3b; however, the two fH variants show no differences in decay accelerating activity. From these data, we conclude that the protective effect of the fH-Ile62 variant is due to its better capacity to bind C3b, inhibit proconvertase formation and catalyze inactivation of fluid-phase and surface-bound C3b. This demonstration of the functional consequences of the fH-Ile62 polymorphism provides relevant insights into the complement regulatory activities of fH that will be useful in disease prediction and future development of effective therapeutics for disorders caused by complement dysregulation.
Complement is a major component of innate immunity with crucial roles in microbial killing, apoptotic cell clearance and immune complex handling. Activation of complement by foreign surfaces (alternative pathway, AP), antibody (classical pathway, CP) or mannan (lectin pathway; LP) causes target opsonization, leucocyte recruitment, and cell lysis. The critical steps in complement activation are the formation of unstable protease complexes, named C3-convertases (AP, C3bBb; CP/LP, C4b2a) and the cleavage of C3 to generate C3b. Convertase-generated C3b can form more AP C3 convertase, providing exponential amplification to the initial activation. Binding of C3b to the C3-convertases generates the C5-convertases with the capacity to bind and cleave C5, initiating formation of the lytic membrane attack complex (MAC).
Nascent C3b binds indiscriminately to pathogens and adjacent host cells. To prevent damage to self and to avoid wasteful consumption of components, complement is under the control of multiple regulatory proteins that limit complement activation by inactivating C3b or C4b, dissociating the multimolecular C3/C5 convertases or inhibiting MAC formation. In health, activation of C3 in the blood is kept at a low level and deposition of C3b and further activation of complement is limited to the surface of pathogens (1).
Factor H (fH) is a relatively abundant plasma protein that is essential to maintain complement homeostasis and to restrict the action of complement to activating surfaces. fH binds to C3b, accelerates the decay of the AP C3 convertase (C3bBb) and acts as a cofactor for the factor I (fI)-mediated proteolytic inactivation of C3b (2–4). fH regulates complement both in fluid phase and on cellular surfaces (5–7). The fH molecule is a single polypeptide chain glycoprotein of 155 kDa composed of 20 repetitive units of ∼60 amino acids (8), named short consensus repeats (SCR), arranged end-to-end like ‘beads on a string’. fH presents different interaction sites for C3b and polyanions which delineate distinct functional domains at the N- and C-termini. The C3b binding site in SCR1-4 is the only site essential for the C3 convertase decay accelerating and fI cofactor activities of fH. Similarly, the C3b/polyanion binding site located within SCR19–20 is the most important site for preventing AP activation through binding to host cell membranes (9).
Several reports in the last few years have established that membranoproliferative glomerulonephritis type II or dense deposit disease (MPGN2/DDD) (10–13), atypical haemolytic uraemic syndrome (aHUS) (14–17) and age-related macular degeneration (AMD) (18–21) are each associated with mutations or polymorphisms in the CFH gene. The available data support the hypothesis that AP dysregulation is a unifying pathogenetic feature of these diverse conditions. They also illustrate a remarkable genotype–phenotype correlation in which distinct genetic variations at CFH specifically predispose to aHUS, AMD or MPGN2. In addition to these CFH variants conferring increased risk to disease, one common extended haplotype in the CFH gene has been described associated with lower risk to aHUS, AMD and MPGN2/DDD (18,22). This CFH haplotype carries the Ile62 variant within the SCR1 domain in the N-terminal region that is essential for fH regulatory activities. It is, therefore, possible that the substitution of Val for Ile at position 62 may increase the fH regulatory activity and thus confer lower risk to AMD, MPGN2/DDD and aHUS by reducing AP activation.
To test this hypothesis, we have purified the two fH variants from the plasma of fH-Val62 and fH-Ile62 homozygote donors and performed a series of binding and functional analyses. Our data show that the fH-Ile62 variant exhibits increased binding to C3b compared with fH-Val62 and is also a more efficient cofactor for fI in the proteolytic inactivation of C3b. Together these data provide an explanation for why fH-Ile62 protects from diseases associated with AP dysregulation.
Interaction of fH-Ile62 and fH-Val62 with surface-bound C3b
Purified C3b was immobilized on microtiter plates and serial dilutions of fH-Ile62 or fH-Val62 variants, ‘polished’ free from potential aggregates by gel filtration, were allowed to interact with C3b for 2 h at 37°C. The fH bound to C3b was detected using an anti-fH mAb (35H9) that recognises equally both variants as described in Materials and Methods section. Binding of the protective fH-Ile62 variant to surface-bound C3b was significantly higher than that of the fH-Val62 variant (P < 0.0001) (Fig. 1A). These data suggest that the Val62Ile polymorphism influences the interaction between fH and C3b. To confirm these findings in a different assay, we performed surface plasmon resonance (SPR) studies using chips coated with identical amounts of fH-Ile62 or fH-Val62 variants and flowed increasing concentrations of C3b. These SPR assays replicated and extended the findings from ELISA experiments, showing that fH-Ile62 binds C3b with a higher affinity than fH-Val62 (Fig. 2A). Steady-state analysis under defined buffer conditions gave a KD of 1.04 µm for fH-Ile62 and 1.33 µm for fH-Val62 (Fig. 2B).
Cofactor activity for fI-mediated proteolysis of fluid phase C3b
In order to study the fI cofactor activity of the fH-Ile62 and fH-Val62 variants, we first performed a fluid phase cofactor activity assay. Identical amounts of purified fH-Ile62 and fH-Val62 variants were added to purified C3b in the presence of fI and incubated for 2.5, 5, 7.5 and 10 min at 37°C. Under the conditions of these experiments, 100% of C3b cleavage was reached after 20 min of incubation. Controls for 0% cleavage were obtained in the absence of fI. The ratio between α′-chain and β-chain of C3b, determined by densitometry, was used to determine the percentage of C3b cleavage. Figure 3A illustrates one experiment representative of several, showing that the fH-Ile62 variant is more efficient as a cofactor for fI in the cleavage of C3b in the fluid phase. Figure 3B shows a significant difference (P = 0.0012) in the % C3b cleavage catalyzed by identical amounts of purified fH-Ile62 and fH-Val62 variants at different incubation times. Figure 3C shows the densitometry analysis for the differences in cofactor activities between the fH-Ile62 and fH-Val62 variants at 6 min incubation time in an independent set of assays. From these experiments, it was calculated that fH-Ile62 is ∼20% more active than fH-Val62 as a cofactor for the fI-mediated cleavage of fluid phase C3b.
Cofactor activity of fI-mediated inactivation of surface-bound C3b
To determine whether the fH-Ile62 variant is also more active than fH-Val62 as cofactor for the fI-mediated inactivation of surface-bound C3b, we used a haemolytic assay. C3b deposited onto sheep erythrocytes (EA) was subjected to degradation by fI in the presence of increasing amounts of purified fH-Ile62 or fH-Val62. For each fH concentration, the residual surface-bound C3b was determined by measuring sheep EA lysis after lytic pathway reconstitution (see Materials and Methods).
Three different experiments, each in triplicate, were performed with identical results (Fig. 4). Calculated EC50 was 14 and 22.6 nm for fH-Ile62 and fH-Val62, respectively. These experiments consistently show that fH-Ile62 is significantly more active than fH-Val62 as a cofactor for the fI-mediated proteolysis of surface-bound C3b (P = 0.0025; two-tailed unpaired t-test). From these experiments, it was estimated that the dose of fH-Val62 needed to achieve 50% fI-mediated inactivation of C3b is 1.6–1.8-fold that required when fH-Ile62 is used.
Decay accelerating activity of the AP C3 convertase
To measure AP convertase decay accelerating activity of the fH-Ile62 and fH-Val62 variants, sheep EA were coated with AP convertase (C3bBb) and incubated with increasing amounts of purified fH-Ile62 or fH-Val62 in the absence of fI. Residual AP convertase on the sheep EA was determined by measuring EA lysis after lytic pathway reconstitution (see Materials and Methods). In three independent experiments, these haemolytic assays showed that fH-Ile62 and fH-Val62 have equivalent decay accelerating activity (Fig. 5A). Independent confirmation of this finding was sought using Biacore (Fig. 5B). AP C3 convertase was assembled on a C3b-coated chip and allowed to decay naturally for 160 s; fH-Ile62 or fH-Val62 at a concentration of 73 nm was then flowed over the chip. Binding of fH and accelerated convertase decay occurred simultaneously. Following dissociation of fH from the surface, remaining convertase was measured; this was identical for each fH variant. Note the increased binding of fH-Ile62 to the surface in agreement with Figure 2A.
Competition between fH and fB for binding to C3b
From the experiments presented above, it is clear that the differences in binding affinity for C3b of the fH-Ile62 and fH-Val62 variants affect their capacity to function as cofactor for fI in the proteolysis of C3b. To explore whether these differences in affinity also influence the ability of fH to prevent formation of the C3 proconvertase by competing with factor B (fB) for binding to C3b competition assays were performed on Biacore. We first showed, in keeping with previous reports, that fH does not accelerate decay of the pre-formed proconvertase C3bB (Fig. 6A). When fB together with increasing amounts of fH was flowed over a C3b surface, competition between fB and fH for binding to C3b was apparent from the fH-dependent decrease in the formation of proconvertase measured following dissociation of fH (Fig. 6B). Next, fB was flowed over C3b and binding competed using identical amounts of the fH-Ile62 and fH-Val62 variants. As expected, fH-Ile62, shown to bind better to C3b, was a more efficient competitor and caused a small but consistent decreased formation of the proconvertase (Fig. 6C). These data illustrate that the increased C3b binding affinity of the fH-Ile62 variant makes it not only a better cofactor for the fI-dependent inactivation of C3b, but also a more efficient inhibitor of the formation of the C3 proconvertase.
Combined effects of the fH Val62Ile and fB Arg32Gln polymorphisms in the formation of the AP C3 convertase
Previously, we have characterized the common fB polymorphism, fB-Arg32/fB-Gln32/fB-Trp32, and found that the AMD-protective allele fB-Gln32 had decreased affinity for C3b compared with the fB-Arg32 and fB-Trp32 alleles. SPR comparison revealed markedly different proenzyme formation activities; fB-Arg32 bound C3b with 4-fold higher affinity than fB-Gln32, and formation of activated convertase was enhanced (23). Here we tested combinations of these two variants of fB with the two variants of fH characterized above in order to explore the consequences of different combinations of variant components and regulators. In haemolytic assays, we found that the combinations complemented each other as predicted from their individual activities (Fig. 7). The fH-Ile62–fB-Gln32 combination was the least lytic and the fH-Val62–fB-Arg32 combination the most lytic (Fig. 7). Calculated EC50s were 4.3 and 3.5 nm (for the fH-Ile62–fB-Gln32 and fH-Val62–fB-Gln32 combinations, respectively) and 3 and 2.1 nm (for the fH-Ile62–fB-Arg32 and fH-Val62–fB-Arg32 combinations, respectively). Differences in the EC50 were statistically significant between the combinations fH-Val62–fB-Arg32 and fH-Ile62–fB-Gln32 (P < 0.001); fH-Val62–fB-Arg32 and fH-Ile62–fB-Arg32 (P = 0.004) and fH-Val62–fB-Gln32 and fH-Ile62–fB-Gln32 (P = 0.034). P-values were calculated using a two-tailed unpaired t-test. No significant differences were observed between the combinations fH-Val62–fB-Gln32 and fH-Ile62–fB-Arg32.
fH plays a key role in regulating the AP by acting as a cofactor for fI-mediated cleavage of C3b to iC3b, by accelerating the dissociation of the AP C3 convertases and by competing with fB for binding to C3b in proconvertase formation (9). All these activities are mediated by the interaction between fH and C3b. Functional studies using truncated molecules have demonstrated that fH possesses binding sites for C3b located at the N terminus (SCR1–4), the C terminus (SCR19–20) and in the middle of the molecule (SCR7) (24,25). The C3b binding sites at the C-terminal and N-terminal ends are well characterized, whereas that in SCR7 is a very weak binding site of unknown function. The C3b binding site in SCR19–20 shows the highest affinity for C3b and plays a critical role in the recognition of foreign surfaces by fH. At the other end of the molecule, the C3b binding site in SCR1–4 is essential for the regulatory activities of fH as it carries the fI-mediated cofactor and decay-accelerating activities of fH. Deletion mutagenesis studies have demonstrated that the N-terminal four SCRs are necessary and sufficient for these activities of fH, suggesting that multiple interactions occur between C3b and the N-terminal region of fH (26,27).
Here we report that the Val62Ile substitution in SCR1 of fH increases its affinity for C3b; as a consequence, when compared with fH-Val62, fH-Ile62 competes more efficiently with fB for C3b binding in proconvertase formation and acquires enhanced cofactor activity for the factor-I mediated cleavage of C3b proteolysis; however, its decay accelerating activity is not altered. These findings show that fH-Ile62 is a better AP convertase inhibitor and provide an explanation for the association of the fH-Ile62 variant with protection in three distinct disorders linked by AP dysregulation. The fact that the Val62Ile substitution affects binding to C3b but not decay accelerating activity suggests that different regions in fH may be involved in binding C3b/cofactor activity and in decay accelerating activity.
SCR1 is necessary for both cofactor and decay accelerating activities (26,27). Our findings imply that the C3b binding site in SCR1 is not directly involved in decay accelerating activity and that SCR1 may contain distinct, although perhaps overlapping, sites for cofactor and decay accelerating activities. This scenario dictates that the interactions of fH with C3b and with C3bBb are structurally distinct. Previously, we showed that the aHUS-associated fB mutation, K323E, located remote from the C3b-fB interaction site, makes the C3bBb convertase resistant to decay by decay accelerating factor (DAF) and fH (28,29). The mutation apparently affects a complement regulator binding site in the von Willebrand factor type A domain of fB (28). We have also previously showed that DAF–SCR2 interacts with Bb, whereas DAF–SCR4 interacts with C3b in the C3bBb complex (30). From comparison with DAF, it is likely that decay accelerating activity of fH also requires binding to both Bb and C3b. We suggest that there are two distinct binding sites in SCR1, one including the Val62Ile fH polymorphism that is necessary for cofactor activity, and a second that binds fB at, or close to, K323 in fB that is essential for decay accelerating activity. We also postulate that fH has a C3b binding site in SCR3/SCR4 that contributes to both cofactor and decay accelerating activities.
Overwhelming evidence has associated MPGN2/DDD, aHUS and AMD with mutations or polymorphisms in the CFH gene and provided conclusive data that AP dysregulation is a unifying pathogenetic feature of these diverse conditions (31). However, only MPGN2/DDD and AMD have pathological similarities. Indeed, occasionally, they occur in the same patient (32). The hallmark of AMD is drusen, a complex, complement-containing material that accumulates beneath the retinal pigmented epithelium; in MPGN2/DDD, accumulation of a drusen-like C3 and electron-dense material occurs along the glomerular basement membrane. In contrast to these ‘debris-associated’ conditions, aHUS is characterized by renal endothelial cell injury and thrombosis (thrombotic microangiopathy), resulting in haemolytic anaemia, thrombocytopenia and renal failure. Consistent with these differences, distinct functional alterations in fH associate with pathogenesis in these disorders. Mutations or polymorphisms altering the C3b/polyanions binding site located at the C-terminal region of fH are strongly associated with aHUS, because they impair the capacity of fH to protect host cells but have no effect on fluid-phase fH activities. On the other hand, mutations that disrupt the capacity of fH to inhibit complement activation in plasma result in massive activation of C3 that causes MPGN2/DDD. This clear genotype–phenotype correlation contrasts with the association of the fH Val62Ile polymorphism, associated with lower risk for the three diseases (18,22).
To understand why the fH-Ile62 variant confers protection from aHUS, MPGN2/DDD and AMD, we purified to homogeneity both fH-Val62 and fH-Ile62 variants and compared in a series of functional assays for potential effects on proenzyme formation and cofactor and decay accelerating activities in fluid phase and on cell surfaces. Using four different experimental approaches, we showed that fH-Ile62 binds better to C3b, competes better with fB to reduce proenzyme formation and performs more efficiently as a cofactor of fI in the proteolysis of fluid phase and surface-bound C3b. These enhanced activities explain the protective role of fH-Ile62 both in diseases associated with fluid phase complement dysregulation, like MPGN2/DDD, and membrane-restricted dysregulation as is the case in aHUS.
One important conclusion from this report is that the protective effect of the fH-Ile62 variant is subtle, with alterations in activities of between 20 and 50% depending on the assay used. This is consistent with the recent observation (33) that the Val62Ile polymorphism causes a very minor perturbation in the structure of SCR1, this contrasts with the larger structural disturbance caused by an aHUS-associated mutation (Arg53His) which has detrimental consequences on the functional activities of fH. Nevertheless, the very nature of the complement system will amplify these small effects. Further, as we show here by combining known functional variants in fB with fH-Ile62 and fH-Val62, particular combinations of variants in components and regulators will result in very different AP characteristics, markedly affecting formation and regulation of the AP C3 convertase in plasma and on cell surfaces. Identification of individuals carrying ‘high risk’ or ‘low risk’ combinations (‘complotypes’) of the polymorphic complement component and regulator variants will be of great importance for prediction of disease risk and may also help in diagnosis and choice of treatment for diseases involving complement dysregulation.
MATERIALS AND METHODS
Purification of complement components and activation fragments
Normal healthy volunteers were screened for mutations/polymorphisms in the CFH gene by automatic DNA sequencing of PCR amplified fragments. Genomic DNA was prepared from peripheral blood cells according to standard procedures (34). Each exon of the CFH gene was amplified from genomic DNA by using specific primers derived from the 5′ and 3′ intronic sequences as described (14). Automatic sequencing was performed in an ABI 3730 sequencer using a dye terminator cycle sequencing kit (Applied Biosystems, Foster City, CA, USA).
Factor H was purified from individuals homozygous for either the fH-Ile62 and fH-Val62 variants who were identical at all other amino acid residues. Fresh EDTA plasma (100 ml) was precipitated with 7% polyethylene glycol 8000 overnight at 4°C. The precipitate was re-dissolved in PBS, dialysed extensively against 20 mm Tris–HCl (pH 7.4), 50 mm NaCl, 5 mm EDTA and applied to a heparin-Sepharose column (Heparin 6B Fast Flow, Amersham) equilibrated in the same buffer. The proteins bound to the column were eluted with a 100–200 mm NaCl gradient in 20 mm Tris–HCl, pH 7.4, 5 mm EDTA. Fractions containing fH were identified by sodium dodecyl sulphate–polyacrylamide gel electrophoresis (SDS–PAGE), pooled, dialysed against 20 mm Tris–HCl, pH 7.6, 20 mm NaCl and 10 mm EDTA and applied to a DEAE-Sephacel column. Bound proteins were eluted with a 20–300 mm NaCl gradient. Fractions containing fH were identified by SDS–PAGE, pooled and further purified by gel filtration on a Superose™ 6 10/300 column (GE Healthcare). The fH peak fractions were pooled and stored frozen at −70°C. The fH used in haemolysis assays and Biacore studies was purified by affinity chromatography using immobilized anti-fH (35H9; in house). Protein was eluted with 0.1 m Glycine/HCl pH 2.5 and gel filtered into assay buffer using a Superdex 200 10/300 column (GE Healthcare) immediately prior to analysis. The purity of the final preparations was confirmed by SDS–PAGE. Preparations of fH-Ile62 and fH-Val62 were obtained without any detectable contaminants or aggregates (Fig. 1B).
C3 and fB were purified by affinity chromatography and gel filtration as described previously (28). Concentration of proteins was assessed using absorbance at A280, molarities were calculated using an extinction coefficient for fH of 1.95 (35), for fB of 1.43 and for C3 of 0.98 (coefficients were obtained by using Protean Software, DNAStar). C3b was generated by limited digestion with trypsin or convertase as previously described (28,36) and re-purified by ion exchange and/or gel filtration as described above (GE Healthcare). C3b was obtained without any detectable contaminants or aggregates. Factor I, factor D and properdin were purchased from Comptech (Tyler, TX, USA).
ELISA C3b binding assay
The binding of fH variants to surface-bound C3b was determined by ELISA. In a 96-well polystyrene microtiter plate, C3b (5 µg/ml) in coupling buffer (0.1 m NaHCO3 pH 9.5) was coated overnight at 4°C. The plate was blocked with washing buffer (20 mm Tris, 150 mm NaCl and 0.1% Tween 20) with 1% bovine serum albumin for 1 h at room temperature (RT). After washing, serial dilutions of fH variants (10 µg/ml) in blocking buffer containing 150 mm NaCl, 5 mm EDTA were added and incubated with surface-bound C3b for 2 h at 37°C. After washing, the plate was incubated with anti-fH monoclonal antibody (mAb) 35H9 (in house) in blocking buffer, for 1 h at RT, and then with a secondary antibody coupled with horseradish peroxidase (DAKO). Colour reaction was developed with o-phenylene-diamine (DAKO) and absorbance measured at 492 nm. fH preparations used in the ligand assay were quantified in duplicate in the same ELISA plate using immobilized polyclonal anti-fH antibody to capture fH and the same anti-fH mAb, 35H9, and secondary antibodies to measure the amount of protein. Concentrations of fH were calculated from curves obtained using purified standard samples.
Kinetic analyses (Fig. 2) were carried out on a Biacore T100, all other analyses were carried out using a Biacore 3000 (GE Healthcare). To measure affinity, fH was amine coupled to a CM5 (carboxymethylated dextran) chip as instructed by the manufacturer (NHS/EDC coupling kit). Number of RUs loaded for both variants were 1004RU (fH-Ile62) and 1003RU (fH-Val62). C3b was flowed across the surface at different concentrations and bound protein was allowed to decay naturally, the buffer was 10 mm HEPES pH 7.4, 100 mm NaCl, 0.005% Surfactant P20. Data were collected at 25°C at a flow rate of 30 µl/min and were double-referenced (data from reference cell and blank inject were subtracted) to control for bulk refractive index changes. To calculate KD-values (Fig. 2), we repeated this experiment on three different surfaces: twice with C3b flowing and once with hydrolysed C3 flowing. Pooling the data from different runs is difficult. However, the ratio of the derived KD-values was the same for each run as follows: fH-Ile62 was 0.77, 0.78 or 0.8-fold lower than the fH-Val62 form. We flowed C3b over the surface (rather than fH over C3b) in order to minimize the avidity effects seen when flowing fH over the surface. In order to obtain the best quality data, the C3b was gel-filtered prior to use to remove any aggregates and then used in the experiment without further concentration. The C3b needed to be at a very high concentration pre-filtration in order to achieve 1 mg/ml post-filtration, this was the maximum concentration that we could use without precipitating the protein pre-filtration. Although we did not achieve saturation in these experiments, in each case the concentration of C3b used exceeded the KD-value (2.2-fold for fH-Ile62 and 1.7-fold for fH-Val62).
In the following experiments, the buffer was 10 mm HEPES pH 7.4, 150 mm NaCl, 1 mm Mg2+. To test the decay activity of fH (Fig. 5), fB at 100 µg/ml (1.1 µm) and fD (2 µg/ml) were flowed across the C3b surface to form the AP C3 convertase as previously described (30). The fH variants were subsequently flowed across the C3b surface at 11.3 µg/ml (73 nm) and decay was monitored. To examine competition between fH and fB for binding to C3b (Fig. 6), both proteins were mixed at the indicated concentrations and flowed at 30 µl/min across the C3b surface in the absence of fD. To determine whether fH accelerated decay of the proenzyme, fH was flowed over the surface subsequent to the fB injection rather than being premixed.
Cofactor activity for fI-mediated proteolysis of fluid phase C3b
The fluid-phase cofactor activity of fH was determined in a C3b proteolysis assay using purified proteins. In brief, C3b, fH and fI were mixed in 10 mm HEPES pH 7.5, 150 mm NaCl, 0.02% Tween 20 at final concentrations of 50 µg/ml (263 nm), 4 µg/ml (25.8 nm) and 10 µg/ml (114 nm), respectively. Mixtures were incubated at 37°C in a water bath and 20 µl aliquots were collected at 2.5, 5, 7.5 and 10 min. The reaction was stopped by the addition of 3 µl of SDS sample buffer (2% SDS, 62.5 mm Tris, 10% Glycerol, 0.75% Bromophenol Blue). Samples were analyzed in 10% SDS–PAGE under reducing conditions. Gels were stained with Coomassie brilliant blue R-250 (BioRad) and proteolysis of C3b determined by measuring the cleavage of the α′-chain using a GS-800 calibrated densitometer (BioRad) and the MultiGauge software package (FUJIFILM). The C3b β-chain was used as an internal control to normalize the % of cleavage between samples. Percentage of cleavage was determined by the ratio between α′-chain/β-chain of C3b and setting as 0% the amount of α′-chain at time 0.
fH-dependent haemolysis assays
Normal human serum (NHS) was sequentially depleted of fB and fH (NHSΔBΔH) by flowing over immobilized anti-Bb (JC1 mAb; in house) and immobilized anti-fH (35H9; in house) affinity columns in complement fixation diluent (CFD; Oxoid), undiluted depleted serum was pooled and used in haemolysis assays as described below. Antibody-coated sheep EA were prepared by incubating sheep E (2% v/v) with Amboceptor (1/1000 dilution; Behring Diagnostics) in CFD (Oxoid) for 30 min at 37°C, EA were washed and resuspended at 2% (v/v) in CFD. To deposit C3b on the E surface (E-C3b), equal volumes of EA and NHSΔBΔH (8% v/v) were incubated at 37°C for 10 min, the C5 inhibitor (OmCI; 6 µg/ml; gifted from Varleigh Ltd, Jersey (37) was added to block the terminal pathway).
To test fH-dependent decay accelerating activity, washed E-C3b cells were resuspended to 2% (v/v) in AP buffer (5 mm sodium barbitone pH 7.4, 150 mm NaCl, 7 mm MgCl2, 10 mm EGTA) and AP convertase was formed on the cell surface by incubating with fB 42 µg/ml (0.46 µm) and fD (0.4 µg/ml) at 37°C for 15 min. PBS/0.25 m EDTA (4% v/v) was added to prevent further enzyme formation and cells (50 µl) were mixed and incubated with 50 µl of fH [serial dilution from 15.4 µg/ml (99 nm)] in PBS/10 mm EDTA for 12 min. Lysis was developed by adding 50 µl NHSΔBΔH (4%, v/v) in PBS/EDTA and incubating at 37°C for 20 min. To calculate lysis, cells were pelleted by centrifugation, and haemoglobin release was measured by absorbance at 415 nm. Control incubations included 0% lysis (buffer only) and 100% lysis (0.1% Nonidet-P40). Percentage lysis 100 × (A415 test sample−A415 0% control)/(A415 100% control−A415 0% control).
To test fH cofactor activity, washed EA-C3b cells were resuspended to 2% in AP buffer and incubated with an equal volume of different concentrations of fH as indicated and constant fI (2.5 µg/ml) for 7 min at 22°C. After three washes in AP buffer, 50 µl cells (2%) were mixed with 50 µl of 70 µg/ml fB (0.75 µm; fB32R or fB32Q) and fD (0.4 µg/ml) and incubated for 10 min at 22°C to form convertase on residual C3b (EA-C3bBb). Lysis was developed by adding 50 µl NHSΔBΔH (4%, v/v) in PBS/EDTA and incubating at 37°C for 20 min. Percentage lysis was calculated as described above.
To assess the effect on lysis by combining different polymorphic variants of fB and fH, the above two assays were combined and modified as follows. EA-C3b cells were incubated with 80 ng/ml (0.5 nm) fH-Ile62 or fH-Val62 variant and 2.5 µg/ml fI for 7 min at 22°C. Washed cells were incubated as described above with different concentrations of fBArg32 or fBGln32, fD and properdin (1 µg/ml) and lysis was developed using NHSΔBΔH.
C.L.H., B.P.M. and S.R.deC. designed research, analysed the data and wrote the paper. C.L.H. and S.R.deC. contribute equally to this work. A.T., T.M. and R.M.B. prepared the proteins. A.T. and C.L.H. performed the binding and functional assays.
Conflicts of Interest statement. None declared.
This work was supported by MRC Project Grant Ref 84908 (to C.L.H. and B.P.M.), Ministerio de Ciencia e Innovación Ref SAF 2005-00913 (to S.R.deC.) the CIBER de Enfermedades Raras and Fundación Renal Iñigo Alvarez de Toledo (to S.R.deC.). We thank the blood donors for their invaluable contribution to the project.