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Complement fixation test
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| Purpose | detects specific antigen or antibody |
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The complement fixation test is an immunological medical test that can be used to detect the presence of either specific antibody or specific antigen in a patient's serum, based on whether complement fixation occurs. It was widely used to diagnose infections, particularly with microbes that are not easily detected by culture methods, and in rheumatic diseases. However, in clinical diagnostics labs it has been largely superseded by other serological methods such as ELISA and by DNA-based methods of pathogen detection, particularly PCR.
Process
[edit]The complement system is a system of serum proteins that react with antigen-antibody complexes. If this reaction occurs on a cell surface, it will result in the formation of trans-membrane pores and therefore destruction of the cell. The basic steps of a complement fixation test are as follows:[1]
- Serum is separated from the patient.
- Patients naturally have different levels of complement proteins in their serum. To negate any effects this might have on the test, the complement proteins in the patient's serum must be destroyed and replaced by a known amount of standardized complement proteins.
- The serum is heated in such a way that all of the complement proteins—but none of the antibodies—within it are destroyed. (This is possible because complement proteins are much more susceptible to destruction by heat than antibodies.)
- A known amount of standard complement proteins are added to the serum. (These proteins are frequently obtained from guinea pig serum.)
- The antigen of interest is added to the serum.
- Sheep red blood cells (sRBCs)[2] which have been pre-bound to anti-sRBC antibodies are added to the serum. The test is considered negative if the solution turns pink at this point and positive otherwise.
If the patient's serum contains antibodies against the antigen of interest, they will bind to the antigen in step 3 to form antigen-antibody complexes. The complement proteins will react with these complexes and be depleted. Thus when the sRBC-antibody complexes are added in step 4, there will be no complement left in the serum. However, if no antibodies against the antigen of interest are present, the complement will not be depleted and it will react with the sRBC-antibody complexes added in step 4, lysing the sRBCs and spilling their contents into the solution, thereby turning the solution pink.[1]
Testing for antigen
[edit]While detection of antibodies is the most common test format, it is equally possible to test for the presence of antigen. In this case, the patient's serum is supplemented with specific antibody to induce formation of complexes; addition of complement and indicator sRBC is performed as before.[citation needed]
Semi-quantitative testing
[edit]The test can be made quantitative by setting up a series of dilutions of patient serum and determining the highest dilution factor that will still yield a positive CF test. This dilution factor corresponds to the titer.[citation needed]
References
[edit]- ^ a b "Animation Quiz 4 - Complement Fixation Test". highered.mheducation.com.
- ^ C. Vaman Rao (2005). Immunology: a textbook. Alpha Science Int'l Ltd. pp. 112–. ISBN 978-1-84265-255-8. Retrieved 3 December 2010.
External links
[edit]- Complement+Fixation+Tests at the U.S. National Library of Medicine Medical Subject Headings (MeSH)
Complement fixation test
View on Grokipediafrom Grokipedia
The complement fixation test (CFT) is a classical serological assay designed to detect specific antibodies or antigens in patient serum by assessing the consumption of complement proteins during antigen-antibody interactions.[1] In this test, patient serum is mixed with a known antigen and a standardized amount of complement; if specific antibodies are present, they bind the antigen and activate the classical complement pathway, fixing (consuming) the complement and preventing subsequent hemolysis of indicator sheep red blood cells (SRBCs) sensitized with anti-SRBC antibody (hemolysin).[1] Conversely, in the absence of specific antibodies, complement remains active and lyses the indicator SRBCs, producing a visible red color in the supernatant, with results typically interpreted as positive if hemolysis is less than 30% at a given serum dilution.[1] The endpoint titer is defined as the reciprocal of the highest serum dilution showing fixation (no or minimal hemolysis).[1]
Developed in 1901 by Belgian bacteriologist Jules Bordet and his colleague Octave Gengou following Bordet's earlier discovery of complement-mediated hemolysis in 1899, the CFT revolutionized diagnostic immunology by providing a quantitative method to measure humoral immune responses.[1] It was first applied to detect antibodies against pathogens like Treponema pallidum in syphilis diagnosis and later standardized by the U.S. Centers for Disease Control and Prevention (CDC) in 1965 as the Laboratory Branch Complement Fixation (LBCF) method to ensure reproducibility across laboratories.[1] The test primarily detects complement-fixing antibodies of the IgM and certain IgG subclasses (IgG1 and IgG3), making it sensitive to early immune responses but less so to IgA or non-complement-activating IgG isotypes.[1]
In clinical practice, the CFT has been widely used for diagnosing and monitoring infectious diseases, including bacterial infections like brucellosis and Q fever (Coxiella burnetii), viral infections such as influenza and hepatitis, and systemic mycoses like histoplasmosis, coccidioidomycosis, and aspergillosis.[1][2]
Despite its historical significance, the CFT has limitations, including subjectivity in visual hemolysis assessment (leading to inter-technologist variability with coefficients of variation up to 60%), requirement for fresh complement sources, and potential interference from anticomplementary factors in serum.[1] Modern adaptations, such as enzyme-labeled or spectrophotometric variants, aim to enhance precision and automation, though it has largely been supplanted by more sensitive assays like ELISA for routine use.[1] Nonetheless, the CFT remains a gold standard for certain regulatory and international trade confirmations, such as in veterinary diagnostics for brucellosis.[2]
Serial dilutions of the patient's heat-inactivated serum (ranging from 1:5 to 1:512) are prepared in VBS and mixed with a standardized amount of antigen in the wells.[3] The mixture is incubated for 30-60 minutes at 37°C to allow formation of antigen-antibody complexes if specific antibodies are present.[34] Phase 2: Complement Addition
A fixed, limited quantity of guinea pig complement (typically 2-3 hemolytic units, HD50) is added to each well.[33] The plates are incubated for 30 minutes at 37°C, during which any formed antigen-antibody complexes fix the complement, depleting it from the solution.[35] Phase 3: Indicator Addition
Sensitized sheep RBCs (coated with anti-sheep hemolysin) are added to all wells.[34] The plates are incubated for 60 minutes at 37°C, followed by 30 minutes at 4°C to allow settling.[33] Hemolysis occurs if complement remains free, lysing the indicator RBCs; no hemolysis indicates fixation by specific antibodies.[3] Endpoint Determination
Results are visually graded on a 0-4+ scale, where 0 represents complete lysis (100% hemolysis, negative) and 4+ represents no lysis (0% hemolysis, positive).[33] The test is considered positive at the highest serum dilution showing approximately 50% lysis (grade 2).[34] Essential controls are included to validate the test: a serum control (serum without antigen to check for anticomplementary activity), a complement control (VBS with complement and indicator to confirm full lysis), and a cell control (RBCs without hemolysin or complement to verify no spontaneous hemolysis).[33] These ensure reagent integrity and absence of non-specific reactions.[3]
Introduction
Definition and overview
The complement fixation test (CFT) is a classical serological assay that detects the presence of specific antigen-antibody complexes by measuring the consumption of complement proteins, which in turn inhibits hemolysis in an indicator system.[3] This test leverages the activation of the complement cascade by immune complexes, where bound complement is "fixed" and unavailable for subsequent reactions.[4] As a foundational method in immunology, it provides a quantitative measure of antibody levels through observable endpoints like the degree of red blood cell lysis.[5] Key components of the CFT include the patient's serum, which may contain target antibodies; a known antigen to facilitate complex formation; an exogenous source of complement, typically guinea pig serum; and a hemolytic indicator system composed of sheep red blood cells sensitized with anti-sheep hemolysin (also known as hemolysin).[3] When specific antibodies in the serum bind the antigen, they activate and consume the complement, preventing it from lysing the sensitized indicator cells and resulting in no hemolysis, which signifies a positive test.[4] In the absence of such complexes, complement remains active and causes complete hemolysis.[5] The CFT has been employed to diagnose infectious diseases, including syphilis (via the Wassermann reaction), tuberculosis, and viral infections such as hepatitis A, by detecting specific antibodies or antigens in serum samples.[4] It is particularly useful for confirming immune responses in acute or chronic infections across humans and animals.[3] Developed in the early 20th century, this test established core principles in serology but has largely been supplanted by more sensitive, automated immunoassays like enzyme-linked immunosorbent assay (ELISA) due to its labor-intensive nature and lower throughput.[5]Historical development
The complement fixation test (CFT) was developed in 1901 by Belgian scientists Jules Bordet and Octave Gengou at the Pasteur Institute in Brussels, where they demonstrated that complement could be fixed (consumed) in the presence of specific antigen-antibody complexes, building on earlier work by Emil von Behring on antitoxins and serum therapy for diphtheria.[6] This foundational observation allowed for the indirect detection of immune responses to pathogens, marking a pivotal advancement in serological diagnostics. Bordet and Gengou's experiments involved mixing serum with bacterial antigens and observing complement-mediated hemolysis inhibition, which laid the groundwork for applying the test to infectious diseases.[7] The test's first major clinical application came in 1906 with the Wassermann test, adapted by German bacteriologist August von Wassermann and colleagues for diagnosing syphilis using beef heart extracts as antigens to detect reagin antibodies.[8] This adaptation transformed the CFT from a research tool into a practical diagnostic method, enabling widespread screening for Treponema pallidum infections and influencing public health efforts against sexually transmitted diseases. The success of the Wassermann test spurred further modifications for other pathogens, establishing the CFT as a cornerstone of early 20th-century immunology.[9] By the 1910s and 1920s, the CFT saw broad adoption for diagnosing bacterial and viral infections, including gonorrhea (via gonococcal complement fixation), typhus (distinguishing epidemic from murine forms), and brucellosis (detecting anti-Brucella antibodies in livestock and humans).[10][11] Its use peaked from the 1920s to 1950s, particularly in military and public health laboratories during outbreaks, before being gradually supplanted by more sensitive and automated assays like enzyme-linked immunosorbent assay (ELISA) in the late 20th century due to the CFT's labor-intensive nature, subjective interpretation, and lower sensitivity for certain antigens.[12] Key milestones included World Health Organization efforts in the 1950s to standardize the test for brucellosis through international reference sera, improving reproducibility across global labs. Despite its decline, the CFT persists in niche applications as of 2025, especially in veterinary diagnostics for diseases like brucellosis and anaplasmosis in resource-limited settings where low-cost, equipment-minimal serology remains viable.[13] Modern adaptations, such as in-house protocols for endemic infections, highlight its ongoing utility in areas lacking advanced infrastructure, though it is rarely used for human viral monitoring like HIV or hepatitis due to superior alternatives.[14]Biological principles
The complement system
The complement system comprises approximately 30 plasma and membrane-bound proteins that function as a key effector arm of the innate immune system, enhancing antibody- and cell-mediated responses against pathogens. These proteins orchestrate several critical processes, including opsonization via C3b deposition to facilitate phagocytosis, induction of inflammation through the generation of anaphylatoxins such as C3a and C5a that recruit immune cells, and direct cytolysis by forming pores in target cell membranes.[15][16] The classical pathway, one of three activation routes, is triggered specifically by immune complexes formed between antigens and antibodies, predominantly IgM or IgG isotypes. Activation begins with the recognition subunit C1q binding to the Fc regions of these antibodies, which induces conformational changes that activate the associated serine proteases C1r and C1s within the C1 complex. C1s then proteolytically cleaves C4 into anaphylatoxin C4a and opsonin C4b, as well as C2 into C2a and C2b; the resulting C4b2a complex serves as the C3 convertase, which deposits C3b on surfaces and amplifies the response by cleaving additional C3 molecules.[16][17] Central to the system are the numbered components C1 through C9, with early-acting proteins like C1 (comprising C1q, C1r, and C1s), C4, and C2 being rapidly consumed during the initiation phase, a process termed fixation. The terminal sequence involves C5 through C9, where C5b sequentially recruits C6, C7, C8, and multiple C9 molecules to assemble the membrane attack complex (MAC), a transmembrane channel that disrupts cellular integrity and leads to lysis.[17][16] Complement functionality is quantified using hemolytic assays, where the CH50 value represents the reciprocal of the serum dilution achieving 50% lysis of antibody-coated sheep erythrocytes via the classical pathway, providing a measure of overall activity. Alternative metrics, such as ACH50 for the alternative pathway, assess pathway-specific efficiency. For experimental purposes, complement is typically sourced from guinea pig or human serum; guinea pig serum is favored for its robust classical pathway activity, often 4- to 5-fold higher than human equivalents, and is standardized to deliver 2-5 hemolytic units per assay to ensure reproducibility.[18][19]Antigen-antibody interactions
Antigens are molecules capable of eliciting an immune response, typically foreign substances such as bacterial proteins, viral particles, or other pathogen-derived components that are specifically recognized and bound by antibodies. These interactions form the foundation for immune recognition in serological assays like the complement fixation test. Small, non-immunogenic molecules known as haptens cannot independently stimulate antibody production but become antigenic when attached to larger carrier proteins, enabling the formation of detectable immune complexes.[17] Antibodies, or immunoglobulins, are glycoproteins produced by B cells that recognize antigens through their variable Fab regions. The two primary classes involved in complement-mediated reactions are IgG, a monomeric Y-shaped molecule, and IgM, a pentameric structure with higher valency. The constant Fc region of both IgG and IgM serves as the binding site for the complement component C1q, with IgM's multiple Fc domains providing enhanced avidity for complement recruitment when antigen-bound. Affinity refers to the binding strength of a single antigen-antibody pair, governed by non-covalent forces like hydrogen bonds and van der Waals interactions, while avidity describes the cumulative strength from multiple simultaneous bindings in a multivalent complex.[17] Immune complex formation occurs when multivalent antigens cross-link with bivalent IgG or multivalent IgM, resulting in lattice-like aggregates that stabilize the interaction and position Fc regions for complement engagement. These lattices amplify the signal for immune activation, similar to the cross-linked structures that drive precipitation in solution or agglutination of particles in related assays, thereby serving as precursors for effector functions.[17] In diagnostic contexts, the specificity of antigen-antibody binding is paramount, achieved through the use of purified or standardized antigens to detect targeted antibodies without cross-reactivity. For instance, cardiolipin, a phospholipid antigen combined with cholesterol and lecithin, is employed in tests for syphilis to identify reagin antibodies with high precision.[20] The efficiency of antigen-antibody binding is modulated by environmental factors, including temperature, which is optimal at 37°C to replicate physiological conditions and maximize reaction kinetics; pH, where deviations from neutrality can alter charge interactions; and ionic strength in assay buffers, which influences electrostatic forces and overall binding stability.[21][22]Test mechanism
Core principle of fixation
The core principle of the complement fixation test relies on the ability of antigen-antibody complexes to activate and consume components of the complement system through the classical pathway, thereby depleting available complement and preventing its use in a subsequent hemolytic reaction.[4] In this process, the formation of immune complexes—where antibodies bind specifically to antigens—serves as the trigger, leading to the fixation or consumption of complement proteins. This activation is specific to the classical pathway, distinguishing it from alternative or lectin pathways, and forms the basis for detecting immune responses without directly observing the complexes themselves.[17] The fixation process begins with the recruitment of C1q, the recognition subunit of the C1 complex, which binds to the Fc regions of antibodies (typically IgM or IgG) within the antigen-antibody complex. This binding induces a conformational change that activates C1r and C1s proteases, which in turn cleave C4 into C4a and C4b, and C2 into C2a and C2b. The resulting C4bC2a complex acts as a C3 convertase, cleaving C3 into C3a and C3b, thereby initiating further downstream events. These steps lead to the formation of stable multimolecular complexes on the immune aggregate, consuming early complement components (primarily C1 through C4) and depleting free complement from the system, which inhibits the full lytic cascade.[17][4] In the absence of antigen-antibody complexes, no such activation occurs, leaving complement proteins unbound and available to participate in the lysis of sensitized indicator red blood cells, which signals a negative test result through observable hemolysis.[4] This no-fixation outcome highlights the test's reliance on complement's dual role: consumption in the presence of specific immunity versus preservation for indicator system detection.[17] Quantitatively, the complement titer is defined as the highest dilution of complement source that results in 50% hemolysis of sensitized red blood cells under standard conditions, establishing a baseline for activity measurement. The test typically employs an excess of complement, such as two minimal hemolytic units (the amount causing 50% lysis), to ensure that any fixation by immune complexes fully depletes the reactive pool without baseline limitations.[23][4]Indicator system
The indicator system in the complement fixation test (CFT) employs a hemolytic assay to detect residual complement activity after potential fixation by antigen-antibody complexes, providing a visual readout of the test outcome. It consists of sheep erythrocytes sensitized with rabbit anti-sheep hemolysin, also known as amboceptor, which forms erythrocyte-antibody (EA) complexes that serve as targets for complement-mediated lysis.[18][24] In the absence of complement fixation during the initial test phase, free complement binds to the sensitized sheep erythrocytes, initiating the classical pathway and activating the terminal complement components C5 through C9. This activation leads to the assembly of the membrane attack complex (MAC), a pore-forming structure composed of C5b-9 that inserts into the erythrocyte membrane, causing cell lysis and the release of hemoglobin into the supernatant.[25][26] The resulting hemolysis manifests as a color change from opaque red (due to intact erythrocytes) to clear or pink (from released hemoglobin), which can be observed visually or quantified spectrophotometrically at 405–415 nm for precision.[18] The standard endpoint for assessing complement activity in this system is 50% hemolysis (CH50), where half of the sensitized erythrocytes are lysed, corresponding to the dilution of complement that achieves this level of activity. Sheep erythrocytes are preferred due to their low non-specific reactivity and consistent sensitivity in hemolytic assays, minimizing background lysis.[27][18] Controls are essential to validate the indicator system: a positive control demonstrates complete hemolysis (indicating no prior complement fixation and full complement availability), while a negative control shows no hemolysis (confirming complement consumption by fixation).[28] For sensitization, rabbit anti-sheep hemolysin is titered to a sublytic dose—typically achieving 70–80% sensitization without spontaneous lysis—by incubating a 2–5% suspension of washed sheep erythrocytes with diluted hemolysin (e.g., 1:50 to 1:200) at 37°C for 30 minutes, followed by washing and storage as a 50% suspension in buffer at 4°C for up to several weeks.[18][29]Procedure
Reagents and preparation
The complement fixation test (CFT) requires precise preparation of core reagents to ensure accurate detection of antigen-antibody complexes. Patient serum serves as the primary source of antibodies and must be heat-inactivated at 56°C for 30 minutes to destroy endogenous complement activity, preventing interference with the assay.[30] Standardized antigen, typically prepared as a suspension containing 4-5 complement-fixing units, is used to react with antibodies in the serum; this standardization ensures consistent reactivity without excess that could lead to non-specific fixation.[28] Complement is sourced from guinea pig serum and titrated to provide 2-5 CH50 units (50% hemolytic complement units) in the working dilution, reflecting the amount required for full activation in the indicator system.[31] Indicator reagents are essential for visualizing complement activity through hemolysis. A 2-5% suspension of sheep red blood cells (SRBCs), washed three times in buffer and preserved in solutions like Alsever's, provides the target for complement-mediated lysis.[28] Hemolysin, an anti-SRBC antibody raised in rabbits, is diluted to 1:1000-1:5000 to achieve 5-12 hemolytic doses (HD50), sensitizing the SRBCs for specific complement binding.[32] Buffers and diluents maintain optimal ionic conditions for complement activation. Veronal-buffered saline (VBS), pH 7.3, supplemented with Ca²⁺ and Mg²⁺ ions, is used for all dilutions and washing steps to support the classical complement pathway; serial dilutions of serum and reagents are typically performed in microplates or tubes using this buffer.[33] Quality control measures are critical for assay reproducibility and must be conducted daily. Antigens are titrated to the highest non-lytic dose that fixes complement in the presence of positive control serum, while complement is titrated to the 100% hemolytic unit (full lysis endpoint) using sensitized SRBCs.[28] Safety protocols and storage conditions minimize risks and preserve reagent integrity. Serum samples require biohazard handling due to potential pathogens, with gloves and biosafety level 2 practices recommended; reagents like antigen and complement are stored at 4°C, while SRBCs are kept at -70°C to prevent degradation, and all manipulations must avoid contamination through sterile techniques.[33]Step-by-step protocol
The standard complement fixation test follows a sequential three-phase protocol performed in 96-well microplates for high-throughput analysis, typically taking 3-4 hours using the warm fixation method.[33] The procedure assumes pre-prepared reagents such as Veronal buffered saline (VBS), antigen, guinea pig complement, and sensitized sheep red blood cells (RBCs).[34] Phase 1: SensitizationSerial dilutions of the patient's heat-inactivated serum (ranging from 1:5 to 1:512) are prepared in VBS and mixed with a standardized amount of antigen in the wells.[3] The mixture is incubated for 30-60 minutes at 37°C to allow formation of antigen-antibody complexes if specific antibodies are present.[34] Phase 2: Complement Addition
A fixed, limited quantity of guinea pig complement (typically 2-3 hemolytic units, HD50) is added to each well.[33] The plates are incubated for 30 minutes at 37°C, during which any formed antigen-antibody complexes fix the complement, depleting it from the solution.[35] Phase 3: Indicator Addition
Sensitized sheep RBCs (coated with anti-sheep hemolysin) are added to all wells.[34] The plates are incubated for 60 minutes at 37°C, followed by 30 minutes at 4°C to allow settling.[33] Hemolysis occurs if complement remains free, lysing the indicator RBCs; no hemolysis indicates fixation by specific antibodies.[3] Endpoint Determination
Results are visually graded on a 0-4+ scale, where 0 represents complete lysis (100% hemolysis, negative) and 4+ represents no lysis (0% hemolysis, positive).[33] The test is considered positive at the highest serum dilution showing approximately 50% lysis (grade 2).[34] Essential controls are included to validate the test: a serum control (serum without antigen to check for anticomplementary activity), a complement control (VBS with complement and indicator to confirm full lysis), and a cell control (RBCs without hemolysin or complement to verify no spontaneous hemolysis).[33] These ensure reagent integrity and absence of non-specific reactions.[3]