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In the leukocyte adhesion deficiency (LAD)-1 syndrome, there is diminished expression of β2(CD18) integrins. This is caused by lesions in the β2-subunit gene and gives rise to recurrent bacterial infections, impaired pus formation, and poor wound healing. We describe a patient with clinical features compatible with a moderately severe phenotype of LAD-1 but who expresses the β2 integrins lymphocyte function– associated molecule (LFA)-1 and Mac-1 at 40%–60% of normal levels. This level of expression should be adequate for normal integrin function, but both the patient's Mac-1 on neutrophils and LFA-1 on T cells failed to bind ligands such as fibrinogen and intercellular adhesion molecule (ICAM)-1, respectively, or to display a β2-integrin activation epitope after adhesion-inducing stimuli. Unexpectedly, divalent cation treatment induced the patient's T cells to bind to ICAM-2 and ICAM-3. Sequencing of the patient's two CD18 alleles revealed the mutations S138P and G273R. Both mutations are in the β2-subunit conserved domain, with S138P a putative divalent cation coordinating residue in the metal ion–dependent adhesion site (MIDAS) motif. After K562 cell transfection with α subunits, the mutated S138P β subunit was coexpressed but did not support function, whereas the G273R mutant was not expressed. In summary, the patient described here exhibits failure of the β2 integrins to function despite adequate levels of cell-surface expression.
The adhesive response of circulating leukocytes to inflammatory stimuli is now well documented (1, 2). After such signals, leukocytes adhere to the blood vasculature using selectin-mediated interactions, and this stage leads to activation of their integrins. The β2 or leukocyte integrins lymphocyte function-associated molecule (LFA)-1 (CD11a/CD18) has a major role in the firm adhesion of leukocytes to endothelium and in their migration across this barrier. In addition, LFA-1 cooperates with the T-cell receptor in antigen-stimulated T-cell priming (3) and, in general, participates in the formation of leukocyte–leukocyte contacts. Mac-1 (CD11b/CD18) is a major phagocytic receptor operating in association with the third β2 integrin, p150,95 (CD11c/CD18), and both recognize as ligands fibrinogen and the complement fragment iC3b (4, 5).
Expression of integrins on the cell membrane is not a guarantee of their ability to function as adhesion receptors. Integrins must undergo conversion from inactive to active ligand-binding status, which occurs through a process of clustering and/or altered conformation (6, 7). The stimulus for this activation is initiated by the triggering of other membrane receptors, a route of signal transduction that has been termed “inside out” signaling. The integrins bind divalent cations such as Mg2+ or Mn2+ in order to function, and an alternative means of directly altering integrin activity is through extracellular exposure to these cations. It is thought that these latter procedures mimic the conformational changes brought about by integrin-activating signals generated intracellularly. Special anti-integrin monoclonal antibodies (MABs) can serve as reporters of this activation. For example, MAB 24 recognizes an epitope on high-affinity β2 integrin (7) and detects a conformational change in the form of interdomain movement involving the ligand binding I domain on the integrin α subunit (8).
Valuable information about the functioning of the β2 integrins has come from study of the leukocyte adhesion deficiency (LAD)-1 syndrome. LAD-1 is an autosomal recessive disorder caused by mutation in the CD18 gene on chromosome 21 that leads to absent or aberrant biosynthesis of the β2 subunit of leukocyte integrins (9–11). This lesion is reflected in the absence or markedly diminished expression on the leukocyte cell surface of the β2 integrins, CD11a/CD18 (LFA-1), CD11b/CD18 (Mac-1), and CD11c/CD18 (p150,95). The patient phenotype is variable but reflects the level of β2 integrins expressed. Patients with <1% expression suffer from life-threatening infections and require bone marrow transplantation for long-term survival (12). In patients with 1%–10% expression, defects in leukocyte mobility, adherence, and endocytosis lead to periodic periodontitis, skin infections, and retarded wound healing with dysplastic scarring. The heterozygotic relatives of the patients have ~40%–60% normal levels of β2 integrins and are clinically normal (9).
We have identified an unusual patient with β2- integrin expression that resembles that of LAD-1 heterozygotes but with a failure of integrin function and lack of expression of the MAB 24 activation epitope. The Mac-1 integrin on stimulated neutrophils was unable to adhere to ligands such as fibrinogen or to participate in bacterial phagocytosis. LFA-1 on T cells from this patient was unable to recognize its principal ligand, intercellular adhesion molecule (ICAM)-1. The adhesion deficiencies of this patient have provided insight into the functioning of β2 integrins and demonstrated that an LAD syndrome can exist when levels of β2- integrin expression should be compatible with normal function.
MABs used in this study from the authors' laboratories are 38 (CD11a), ICRF44 (CD11b), 3.9 (CD11c), H52 (CD18), 1B4 (CD18), 15.2 (CD54), and MAB 24, directed against an activation reporter epitope on β2 integrins (13), QS4120 (CD4) MAB 14 (CD8), and control MAB 52U. Other MABs were kind gifts as follows: CD11a MAB DF1524 from D. Flavell (Southampton General Hospital, Southampton, United Kingdom); CD18 MABs KIM 127 and KIM 185 from M. Robinson (CellTech, Slough, United Kingdom); MAB 60.3 from Bristol-Myers Squibb Co. (Seattle, Washington, USA); TS2/16 (CD29) and HP1/2 (CD49d) from R. Lobb (Biogen Inc., Cambridge, Massachusetts, USA; HUTS 21 (CD29) directed against an activation reporter epitope on β1 integrins (14) from C. Cabanas (Universidad Complutense, Madrid, Spain); CAL 3.10 (CD50) from D. Simmons (Imperial Cancer Research Fund, Oxford, United Kingdom); UCHT1 (CD3) and UCHL1 (CD45RO) from P. Beverley (University College, London, United Kingdom); MHM24 from A. McMichael (Institute of Molecular Medicine, Oxford, United Kingdom); LPM19c from K. Pulford LRF Diagnostic Unit (Oxford, United Kingdom); and control MAB OX34 from the MRC Cellular Immunology Unit (University of Oxford, Oxford, United Kingdom). Additional CD11 and CD18 MABs were from the Fifth Leukocyte Typing Workshop (Boston, Massachusetts, USA, 1993). Phycoerythrin-conjugated CD18 MAB L130 was purchased from Becton Dickinson UK Ltd. (Oxford, United Kingdom). SAM-1 (CD49e) was purchased from Eurogenetics (Hampton, United Kingdom). Unless otherwise specified, all MABs were purified and used at 10 μg/ml.
Neutrophils were isolated from heparin-anticoagulated venous blood obtained from the patient and age-matched controls by dextran sedimentation and Percoll density gradient centrifugation (15). The neutrophils were removed and washed in HBSS containing 1 mM Ca2+, 1 mM Mg2+, 0.1% wt/vol glucose, and 10 mM HEPES (H-HBSS), and resuspended at 5 × 106/ml. The neutrophils were >95% pure and >99% viable.
Mononuclear cells were obtained from the peripheral blood by centrifugation over Lymphoprep (Nycomed, [U.K.] Ltd., Birmingham, United Kingdom) T lymphoblasts were expanded from these populations by initial activation with 1 μg/ml phytohaemagglutinin (Murex Diagnostics Ltd., Dartford, United Kingdom) for 4 days at 37°C in Roswell Park Memorial Institute medium (RPMI) with 10% FCS, as described previously (16). Cells were then maintained in culture with 20 ng/ml rIL-2 (Cetus Corp., Berkeley, California, USA) and used between days 10 and 14 of culture.
Purified neutrophils and T cells (~5 × 105 cells in 50 μl) were incubated with MABs for 30 min at room temperature or MAB 24 at 37°C in H-HBSS as described previously (17, 18). The cells were washed in FACSwash (PBS with 0.2% wt/vol BSA, 0.1% wt/vol sodium azide) and resuspended in FACSwash containing 1:200 diluted FITC-conjugated goat anti–mouse IgG (Sigma Chemical Co., Poole, United Kingdom). After 30 min on ice, the cells were again washed, resuspended in 200 μl FACSwash, and analyzed using the FACScan BBecton Dickinson [Europe], Meylan, France). K562 transfectants were similarly analyzed. Alternatively, 50-μl samples of blood were incubated for 15 min with 5 μl of phycoerythrin-conjugated MAB L130 (CD18), and the rest of the procedure was carried out as described previously (19). Leukocytes were incubated at 37°C with FITC-conjugated MAB 24 in whole blood using a similar method.
Maxisorp Immuno-plates (96-well; GIBCO BRL, Paisley, Scotland) were coated overnight at 4°C with 50 μl of fibrinogen (Sigma Chemical Co., Dorset, United Kingdom) at 2 mg/ml in 0.1 M carbonate buffer, pH 9.5, and then washed two times in H-HBSS suspension buffer. Purified neutrophils (5 × 106/ml) were labeled with 1 μM 2′,7′-bis-(2-carboxyethyl)-5-(and-6)-carboxyfluorescein-acetoxymethyl ester (BCECF; Calbiochem-Novabiochem UK Ltd., Nottingham, United Kingdom) for 30 min at room temperature (20). After washing, 50 μl of cells (2 × 106/ml) were added to appropriate wells together with 50 μl of either H-HBSS alone or H-HBSS containing 2 × 10–7 M FMLP. After 30 min at room temperature, the plates were washed, and adhering neutrophils were quantified using a fluorescence microtiter plate reader (Fluoroskan II; Labsystems, Basingstoke, United Kingdom).
A construct encoding the five extracellular domains of human ICAM-1 fused to the Fc portion of human IgG1 (ICAM-1/Fc) was prepared as described previously (21). ICAM-2/Fc and ICAM-3/Fc (gift from D. Simmons, Imperial Cancer Research Fund, Oxford, United Kingdom) were similarly prepared. Flat-bottomed 96-well Immulon 1 plates (Dynatech Laboratories Ltd., Billinghurst, United Kingdom) were precoated with 50 μl of ICAM-1/Fc (0.24 μg/well), ICAM-2/Fc (0.5 μg/well), and ICAM-3/Fc (1 μg/well) in PBS overnight at 4°C, blocked with 2.5% (wt/vol) BSA in PBS for 1 h at room temperature, and then washed four times in PBS and twice in 20 mM HEPES, 140 mM NaCl, 2 mg/ml glucose, pH 7.4 (HEPES/NaCl buffer). A total of 5 × 107 cultured T cells were labeled with 25 μCi of [3H]thymidine overnight at 37°C and then washed three times in HEPES/NaCl buffer. On ICAM/Fc–coated wells, 50 μl of T-cell suspension (5 × 106 cells/ml) was combined with 50 μl of HEPES/NaCl buffer containing at two-times concentration 10 mM MgCl2/2 mM EGTA (Mg2+/EGTA), 1 mM Mn2+, 1 mM EDTA, or 100 nM phorbol-12,13-dibutyrate (PDBu; Calbiochem-Novabiochem UK Ltd.). Other integrin-activating protocols included treatment of T cells in RPMI- 1640 with MAB UCHT1 at 10 μg/ml, CD18-activating MABs KIM 127 or KIM 185 at 20 μg/ml, and CD29 MAB TS2/16 at 10 μg/ml as described previously (18). Alternatively, cells were preincubated at 37°C with 5 μM Ca2+ mobilizer thapsigargin (Calbiochem-Novabiochem UK Ltd.) (22). The assay was then performed exactly as described previously (18, 22).
PolyA RNA was obtained from Epstein-Barr virus (EBV)–transformed cells of patient JT (JT-EBV) using the Quickprep Micro mRNA purification kit (Pharmacia Biotech, St. Albans, United Kingdom). The resulting mRNA was used to make cDNA with the Reverse Transcription Kit (Promega Corp., Southampton, United Kingdom). The CD18 cDNA was first amplified with oligonucleotides flanking the coding region (K88/16 and A87/20) using the Expand High Fidelity PCR System (Boehringer Mannheim, East Sussex, United Kingdom). Two overlapping fragments were amplified with the pfu polymerase (Stratagene Ltd., Cambridge, United Kingdom): A (“–73” to “968”) using the oligonucleotides A87/19 and A89/14, and B (“860” to “2400”) using the oligonucleotides K89/17 and F89/11. These fragments were cloned into pBluescript using the pCR-Script Amp SK(+) cloning kit (Stratagene Ltd.). DNA sequencing was performed using reagents in the T7Sequencing Kit (Pharmacia Biotech) on double-strand templates with appropriate primers.
Genomic DNA from JT-EBV–transformed cells was prepared as described previously (23). The region containing the S138P mutation in exon-5 was amplified using nested PCR (24), with the first rounds using oligonucleotides C93/17 and C93/18, and the second rounds using oligonucleotides K89/16 and E90/22. The region containing the G273R mutation in exon-7 was similarly amplified using the oligonucleotide pairs I67 and I78, and E94/04 and E94/03 (24). The PCR fragments were cloned and sequenced.
The sequences of the oligonucleotides are A87/19, CCAGGGCAGACTGGTAGCAAAGCC; I67, GAAACTGAGGCAGGTAACC; I78, GCTCTGTCAGGTGGAGACC; E94/03, TCAGTGGTGTCCTGCCAG; and E94/04, TGCTGGTGTTTGCCACTG. All other oligonucleotides were described previously (25).
Both the S138P and G273R mutations are within a BamHI–EcoRI fragment of the CD18 cDNA. The fragments carrying the mutations were gel purified with the QIAquick Gel Extraction kit (QIAGEN Ltd., Crawley, United Kingdom) and exchanged into the normal CD18 cDNA in the expression vector pcDNA3 (Invitrogen BV, Leek, the Netherlands). cDNA clones for CD11a and CD11b have been described previously (26). K562 were grown in RPMI-1640 with 10% FCS (RPMI/FCS) to log phase and resuspended in serum-free RPMI-1640 at ~1 × 107/ml. A total of 0.5 ml of cells was transferred into a 0.4-cm cuvette, and 40 μg of CD11 cDNA and 10 μg of CD18 cDNA were added. Electroporation was carried out at 960 μF and 320 V (Gene Pulser; Bio-Rad Laboratories Ltd., Hemel Hempsted, United Kingdom) K562 transfectants were allowed to recover in RPMI with 10% FCS at ~2 × 105/ml after electroporation for 24 h at 37°C in 5% CO2 incubator. Surface expression of CD11/CD18 antigens was analyzed by flow cytometry as described for T cells and neutrophils.
A total of 25 ml of cells was spun down, resuspended in 3 ml of RPMI with 5% FCS, 10 mM HEPES, pH 7.5, and labeled by adding 5 μl BCECF (1 μg/ml in DMSO) for 30 min at 37°C. The cells were washed twice in RPMI/FCS/HEPES and resuspended in 2.5 ml together with final concentrations of activating MAB KIM 185 or blocking MABs (either CD11a MAB MHM24 or CD11b MAB 2LPM19c at 10 μg/ml) and 5 mM Mg/1mM EGTA. Next, 50 μl of the cell suspension was delivered into each microtiter well precoated with ligands and was incubated at 37°C for 30 min. The cells were washed three times with 150 μl of RPMI/FCS/HEPES, and the number of cells that remained bound was determined using a fluoroscent plate reader (Cytofluor 4000; PerSeptive Biosystems, Framingham, Massachusetts, USA). Total cells in each well were quantitated before washing.
A total of 100 μl of anti–human IgG (Fc specific) at 5 μg/ml in 50 mM sodium-bicarbonate, pH 9.0, was coated onto each microtiter well for 4 h at room temperature followed by incubation at 4°C overnight. The wells were washed once with 150 μl PBS and blocked with 150 μl of 0.5% (wt/vol) BSA in PBS at 37°C for 45 min. Next, 50 μl of ICAM/Fc (1, 2, or 3) at 1 μg/ml in 0.1% (wt/vol) BSA in PBS was added to each well.
A total of 100 μl of iC3b, a kind gift of A.W. Dodds and R.B. Sim (University of Oxford, Oxford, United Kingdom), at 7.5 μg/ml and BSA at 50 μg/ml in 50 mM sodium-bicarbonate was coated for 4 h at room temperature followed by incubation at 4°C overnight. After washing once with 150 μl PBS, the wells were blocked with 300 μl of 0.2% (wt/vol) polyvinylpyrrolidone (average mol wt = 10,000; Sigma Chemical Co.) in PBS at room temperature for 2 to 3 h. The wells were washed twice with 150 μl of RPMI/FCS/HEPES before use.
We describe 15-year-old patient JT, who first presented as an infant with severe and recurrent skin infections requiring prolonged treatment with intravenous antibiotics and surgery to remove necrotic tissue. In spite of attentive oral hygiene, the patient suffered from severe periodontitis and gingivitis. Otitis media and chest infections had also been consistent features of this patient's condition. Organisms isolated from infected sites included Staphylococcus aureus, Pseudomonas, and Streptococcus species.
The neutrophil count was persistently elevated, reaching peaks of >50 × 109/l at times of infection compared with the range of 2–8 × 109/l among normal individuals. Phagocytosis by the patient's neutrophils was <25% that of a healthy adult control as assessed by internalization of a strain of Staphylococcus epidermidis that was poorly phagocytic in the absence of complement (n = 2). Respiratory burst was either normal or slightly enhanced, and intracellular killing of S. epidermidis was within normal limits. Therefore, although the uptake of the organisms was faulty, intracellular processes by which phagocytes deal with bacteria appeared normal.
Lymphocytes were within the normal range of 1.5 –4 × 109/l, and T-lymphocyte subsets and mitogen and antigen responses were also within normal limits. There was evidence of lymphocyte activation with increased expression of CD25 and decreased expression of L-selectin on CD4 cells. Immunoglobulin levels, resting nitroblue tetrazolium tests, and C-reactive proteins were elevated, consistent with chronic infection. Bleeding time, platelet count, platelet function, and plasma coagulation parameters were all normal. Put together, these clinical features are typical of LAD-1 classified as moderately severe (9), although separation of the patient's umbilical cord, which is a frequent but not invariant feature of LAD-1, was not delayed. Since 1994 the patient's condition deteriorated, with frequent occurrence of sustained skin infections with lesions extending into soft tissues, healing slowly, and leaving dysplastic scars. The severity of these episodes necessitated bone marrow transplantation in the autumn of 1997.
The chief characteristic of LAD-1 is the absence (<1%) in severe cases or reduction (1%–10%) in moderate cases of β2 integrin expression. LAD-1 heterozygotes have ~50% expression of β2 integrins and are clinically normal (9). We first used CD18 MAB L130 in whole blood to measure the patient's β2 integrin levels compared with matched controls. The neutrophil β2 integrin levels were 58% (range 35%–87%) of normal, and the lymphocyte levels were 65% (range 55%–83%) of normal controls (n = 5). The levels of β2 expression varied considerably, undoubtedly due to the immune status of the patient, but the conclusion was that the levels of integrin expressed were similar to those of LAD-1 heterozygotes and should not have given rise to a severe deficiency in leukocyte function.
We next investigated expression of the individual β2 integrins on the patient's resting neutrophils. The patient's levels of LFA-1 (CD11a/CD18) were equivalent to those of control neutrophils, and those of Mac-1 (CD11b/CD18) were ~50% of those expressed by the control neutrophils (Fig. (Fig.11a). This expression of β2 integrins in the face of LAD-1 symptoms suggested that there might be a deficiency in their ability to function. This was tested directly by investigating the Mac-1–dependent adhesion of neutrophils to immobilized ligand fibrinogen. In the presence of formylmethionylleucylphenylalanine (FMLP), the patient's neutrophil Mac-1 displayed no evidence of adhesion to fibrinogen compared with a control (Fig. (Fig.11b), nor to iC3b (data not shown). In fact, background levels of adhesion of the patient's neutrophils were also well below those of the control neutrophils. Other stimulators of β2 integrin adhesion, such as the β2-activating MABs KIM 127 and KIM 185 (27, 28) and treatment with divalent cation Mn2+ (29), failed to induce Mac-1–specific adhesion of neutrophils (data not shown).
MAB 24 is specific for β2 (CD11/CD18) integrins and reacts with an epitope that reports the activation of these integrins after exposure to extracellular cations Mg2+ or Mn2+ (7, 29). On control neutrophils, the MAB 24 epitope was minimally present on resting cells, but expression was increased markedly in response to FMLP. In contrast, no MAB 24 epitope expression was seen in either resting or stimulated neutrophils from the patient (Fig. (Fig.11c). Therefore, in spite of the expression of adequate levels of the major neutrophil integrin Mac-1 (i.e., at the level similar to that found in heterozygote LAD-1 carriers), the patient's neutrophils exhibited a profound failure to function.
As expression of the neutrophil β2 integrins was within expected range for normal function, it was possible that the cells were deficient in their ability to receive activating signals. Neutrophils were examined for other hallmarks of activation such as the upregulation of expression of Mac-1 (30, 31). After stimulation with FMLP, there was a mean increase in Mac-1 of approximately twofold in both purified (Fig. (Fig.11c) and whole-blood neutrophils (data not shown) from control and patient. L-selectin loss, which is another feature of leukocyte activation, was comparably diminished by patient and control cells by FMLP (data not shown). The features indicate that the patient's neutrophils were able to respond to an exogenous activating stimulus in a normal manner.
It was possible that the functional lesion was restricted to neutrophils and that the β2 integrins on other types of leukocytes might function normally. To test this possibility, we investigated the behavior of the β2 integrin LFA-1 and other characteristic T-cell phenotypic markers on the patient's T cells. A comparison of the fluorescence values shows LFA-1 expressed on the patient's T cells after culture to be a mean of 183.4 ± 27.0 (n = 3) compared with 474.4 ± 113.93 (n = 5) on control cells, indicating the level of patient LFA-1 to be ~40% of normal levels. In the samples illustrated in Table Table1,1, the two other β2 integrins, Mac-1 and p150,95, were expressed at negligible levels on both patient and control T cells. MABs detecting other adhesion receptors, such as the β1-integrin subunit (CD29), were present at normal levels on the LAD patient's T cells, as were the LFA-1 ligands ICAM-1 (CD54) and ICAM-3 (CD50). Other markers characteristic of the T cell, such as CD3, CD4, CD8, and CD45RO, were comparable between patient and control T cells (Table (Table11).
The ability of the patient's T-cell LFA-1 to function was investigated by assessing binding activity to immobilized ligand. These T cells, in contrast to control T cells, could not be induced to bind to ICAM-1 after stimulation with a variety of agonists (Fig. (Fig.2).2). Agonists used for stimulation included those that mediate adhesion through intracellular signaling, such as PDBu, CD3 triggering, or the Ca2+ mobilizer thapsigargin (7, 22), and those that induce adhesion from outside the cell by treatment with divalent cations Mg2+/ethyleneglycol-bis (β-aminoethyl ether)-N,N′-tetraacetic acid (EGTA) or Mn2+, as well as the β2 integrin–activating MABs KIM 185 and KIM 127 (28). Adhesion of control T cells to ICAM-1 could be blocked in all cases by MABs specific for both LFA-1 (Fig. (Fig.2)2) and ICAM-1 (data not shown). These results demonstrate that LFA-1 on the patient's T cells is not able to adhere to ICAM-1 in either a constitutive or inducible fashion under a wide variety of adhesion-activating conditions.
Analysis of two other LFA-1 ligands, ICAM-2 and ICAM-3, showed that the patient's T cells could not be induced to adhere to them after PDBu and thapsigargin treatment (Fig. (Fig.33a) as did normal T cells (data not shown). However, they did bind to ICAM-2 and ICAM-3 after treatment with the divalent cations Mg2+/EGTA (Fig. (Fig.33a) or Mn2+ (Fig. (Fig.3,3, b and c), which are considered to activate integrins from the cell exterior by directly altering their conformation (18). The adhesion was specific, as it was blocked by CD11a or CD18 MAB or by chelation of divalent cation with ethylenediaminetetraacetate (EDTA).
To determine whether there was a general defect in integrin function or something more specific to β2 integrins, we examined the ability of β1 receptors on T cells to bind to the extracellular matrix molecule fibronectin. Both control and patient's T cells adhered comparably to fibronectin after stimulation with PDBu, Ca2+ mobilizer thapsigargin, β1 integrin-activating MAB TS2/16, and divalent cations Mn2+ (Fig. (Fig.4,4, a and b) and Mg2+/EGTA (data not shown). The adhesion was completely blocked with MABs to α4 (VLA-4/CD49d) and α5 (VLA-5/CD49e) integrins (Fig. (Fig.44b). Thus, the inability of patient T cells to bind to ICAM-1 does not reflect a general integrin deficiency, because VLA-4 (α4β1) and VLA-5 (α5β1) integrins function normally.
Integrin activity was examined further by investigating induction of activation epitopes. MAB 24, which reports a state of activated β2 integrin, was neither induced on the patient's T cells at 0.5 mM Mn2+ (Fig. (Fig.5)5) nor following titration of either Mn2+ or Mg2+/EGTA up to 10 mM divalent cation (data not shown). In contrast, these levels of cations induced MAB 24 expression on normal T cells. A β1 activation epitope detected with MAB HUTS 21 was induced comparably by 0.5 mM Mn2+ treatment of both normal and patient's T cells (Fig. (Fig.55).
Mutations were identified by sequencing clones of the β2 cDNA fragments A (nt “–73” to “968”) and B (nt “860” to “2400”) (Table (Table2).2). Nine fragment A clones were sequenced and two point mutations were identified. Six of nine clones had the nt change T412C, resulting in amino acid mutation S138P. The other three clones had the nt change G817A, resulting in the amino acid change G273R. Nine fragment B clones were also sequenced; three clones had the nt change C1111A, and the other six, C1323T, with neither change affecting amino acids at V367V and V441V. One clone with each of the A fragments carrying the mutations, and each of the B fragments carrying the polymorphisms, was completely sequenced and no other mutation was found. It was not determined which polymorphism and point mutation were coassociated on the same allele. To verify these cDNA sequencing results, genomic DNA fragments containing the mutations were cloned and sequenced. Of the exon-5 clones, three were normal and three had the mutation S138P. Two exon-7 clones were normal and three had the mutation G273R. Thus, the patient is a compound heterozygote carrying the S138P and G273R mutations in his two CD18 alleles.
The expression of CD11/CD18 antigens on the patient's leukocytes is exceptionally high for patients with LAD-1. It was therefore reasonable to assume that one or potentially both mutations could support CD11/CD18 heterodimer formation. CD11 and CD18 cDNAs were electroporated into K562 cells, and expression was assayed after 24 hours using the CD18-specific MAB 1B4, which recognizes the β2 subunit in heterodimeric form (32) (Law, S.K., unpublished data). It is clear that the S138P mutation can support the formation of LFA-1 and Mac-1 comparably to the wild-type CD18 subunit, whereas G273R cannot (Fig. (Fig.6).6). Identical results were obtained when the transfectants were tested with CD11a MAB MHM24, CD11b MAB 2LPM19c, or a second CD18 MAB H52, and similar results were also obtained after COS cell transfection (data not shown). The transfectants were tested in adhesion assays, using as immobilized ligand ICAM-1, -2, and -3 for LFA-1, and iC3b and denatured bovine serum albumin (BSA) for Mac-1. The wild-type transfectants gave positive adhesion in response to stimulants Mg2+/EGTA and/or the activating CD18 MAB KIM 185, but the α subunits in combination with β2 mutant S138P demonstrated no ability to adhere under any condition of stimulation (Table (Table33).
The LAD known as LAD-1 is caused by reduced β2 integrin expression on leukocytes. LAD-1 has been recognized as a neutrophil disorder because of recurrent life-threatening infections principally due to the lack of the phagocytic receptor Mac-1 (9–11). We describe patient JT, who has all the clinical features of LAD-1 but has expression of the β2 integrins at levels similar to those of LAD-1 heterozygotes, who have ~50% of normal expression but are clinically unaffected. Two novel mutations, S138P and G273R, were identified in the patient's CD18 alleles. We have shown that S138P can support expression of LFA-1 and Mac-1 on K562 transfectants but that the expressed integrin does not function. The G273R mutation supports neither expression nor function of LFA-1 or Mac-1. It is therefore likely that the CD11/CD18 antigens expressed on the patient's leukocytes contain the S138P mutation in the CD18 subunit and that the G273R mutation is responsible for the LAD-1 heterozygote-like levels of expression.
Neither the patient's neutrophils nor K562 transfectants expressing Mac-1(S138P) adhere to Mac-1 ligands fibrinogen and iC3b. However, the patient's T cells have limited CD11a/CD18–mediated adhesive properties. Whereas they do not adhere to ICAM-1 under any of the activation protocols tested, they can adhere to ICAM-2 and ICAM-3 when activated extracellularly with Mg2+/EGTA and Mn2+. This result provides evidence that LFA-1 recognizes each ligand in a unique way and suggests the possibility that there could be a structural defect in the patient's LFA-1 that prevents interaction with ICAM-1 but allows some interaction with ICAM-2 and ICAM-3. There is previous evidence that LFA-1 interacts distinctively with its individual ligands. For example, CD11a MAB MEM-83 induced LFA-1 to selectively bind ICAM-1 but not to ICAM-3 (33, 34), and, conversely, two other CD11a MABs block binding of LFA-1 to ICAM-3 but not to ICAM-1 (34). The binding site for LFA-1 on ICAM-1 is located within the first two domains (21, 35); however, it appears that domain 1 of ICAM-3 is sufficient for LFA-1 binding (36). Electron microscopic evidence shows that for ICAM-3, domain 2 is less structurally dependent on domain 1 than for ICAM-1(35, 37, 38). Another difference is that ICAM-1 is present on the membrane as a dimer (39), whereas at least ICAM-2 appears to be a monomer (40). Finally, the fact that murine LFA-1 can bind human ICAM-2 and ICAM-3, but not ICAM-1, implies that the first two ligands might have structural features in common not shared with ICAM-1 (41). Taken together, the implication of these observations is that the interaction of LFA-1 with ICAM-1 has special features distinct from that interaction with ICAM-2 and ICAM-3.
The patient's EBV-transformed B cells, and K562 transfectants expressing LFA-1(S138P), also failed to adhere to ICAM-1, but, unlike the patient's T cells, they cannot be promoted to adhere to ICAM-2 and ICAM-3 by divalent cation manipulation. This discrepancy may be due to the inability of the EBV-transformed B lymphocytes and the transfectants to respond to the full range of integrin-inducing signals. For example, adhesion to ICAM-2 or ICAM-3 of EBV-transformed B cells from a normal individual, and K562 cells expressing wild-type LFA-1, can only be consistently demonstrated with Mg2+/EGTA in addition to an activating MAB such as KIM 185. In comparison, either Mg2+/EGTA or KIM 185 is sufficient to activate ICAM-1 adhesion (Table (Table33 and ref. 26). The patient's T cells had a completely normal ability to bind to fibronectin via the α4β1 (CD49d/CD29) and α5β1 (CD49e/CD29) integrins. As with other patients with LAD-1, the ability of leukocytes to bind to other integrins such as the fibronectin receptors makes possible lymphocyte responses, and, for this patient, the additional ability of recognizing ICAM-2 and ICAM-3 may also have contributed to his survival into the midteen period.
The mutations found in the β2 subunit of the patient have not been described previously. Both mutations lie in the putative I domain of the integrin β2 subunit. A model of this region of the β2-subunit I domain has two extra β strands between β strand D and helix 5 (42) when compared with a solved α-subunit I-domain structure (43). The G273R mutation that leads to nonexpression of integrin is located in the loop between β strand D and the first extra β strand. No function has yet been assigned to this loop, but it is of interest that G273R mutation affects heterodimer formation.
The S138P mutation is novel in that it gives rise to expression of αβ heterodimer, but these integrins are without function. The S138P mutation is also novel in that it is the first reported natural mutation within the metal ion–dependent adhesion site (MIDAS) motif, which lies between the β strand A and helix 1 of the I-domain model. The divalent cation binding MIDAS-like (DXSXS) motif was initially described in the I domain of the α subunit as the key Mg2+/Mn2+ binding site of the integrin on which ligand binding totally depends (43). It is also appreciated that β subunits contain a MIDAS motif that binds cations and is involved in ligand binding (42–45). The patient's mutated S138P represents the second Ser in the DLSYS of the β2 MIDAS motif. The importance of the conserved residues in DLSYS motif of β2 was studied by mutagenesis in which the D134, S136, and S138 were replaced with Ala in three separate constructs (46). Whereas the D134A and S136A mutants were fully capable of forming LFA-1 and Mac-1, the resultant heterodimers were incapable of binding ICAM-1 and iC3b, respectively. Whether the mutants LFA-1(D134A) and LFA-1(S136A) can bind ICAM-2 and ICAM-3 was not addressed. The S138A mutant, in this same work, was reported to be defective in forming LFA-1 and Mac-1 (46). However, the same mutation was reported to be competent in forming Mac-1 by another group. The Mac-1(S138A) was not adherent to iC3b, denatured ovalbumin, and fibrinogen, but its binding to the neutrophil inhibitory factor was not impaired (47).
Another indicator of the status of integrin function is the expression of integrin “activation reporter” epitopes such as detected by MAB 24 for β2 integrins (7). Expression of this epitope correlates with the increased ability of LFA-1 to bind soluble ICAM-1, which is taken as a measure of high-affinity integrin (7, 18, 48). Expression also correlates with an interdomain movement involving the α subunit I domain that occurs upon binding of Mg2+ (8). The lack of 24 epitope expression by the β2 integrins on the patient's neutrophils and T cells confirmed that these integrins were not undergoing activation and may be deficient in tertiary structural changes necessary for full integrin function. Although Mg2+/EGTA caused neither 24 epitope expression nor adhesion to ICAM-1, it did promote adhesion to ICAM-2 and ICAM-3. The speculation here is that 24 epitope expression may mark an LFA-1 conformation that is specifically required for ICAM-1 binding. In this regard, it is interesting that the mutagenesis of the β3-subunit residue S123A, which corresponds to S138 of β2, is associated with a lack of ability of the integrin αIIbβ3 to undergo conformational change (49).
In summary, we describe a patient expressing adequate levels of β2 integrin but with failure of β2-integrin function that has led to disease that is clinically indistinguishable from a moderately severe form of LAD-1. This patient differs from another recently described variant LAD-1 that has normal CD18 alleles but may have a signaling defect (50). Patient JT is, however, similar to a Glanzmann's thrombasthenia patient who has platelets with heterozygote-like expression of αIIbβ3. On one allele, this patient has a mutation giving rise to a truncated β3 subunit, leading to faulty signaling and loss of function (51). Because patients with defects in integrin function may not be easily recognized by the usual characteristic of absent or low expression, it is presently unknown how common this variant type of lesion might be.
We are extremely grateful to patient JT and his family for their cooperation and support throughout this study and to Gareth Morgan, Mark Peters, and Karolina Kotowicz (Institute of Child Health) for bringing this patient to our attention, performing the platelet studies, and generating the EBV-transformed cell line (JT), respectively. We thank the following for generous gifts of monoclonal antibodies: Peter Beverley, Carlos Cabanas, David Flavell, and Martyn Robinson. Alison McDowall and Matthew Robinson (Imperial Cancer Research Fund, London, United Kingdom) provided extremely helpful comments on this manuscript.