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THE PATHOPHYSIOLOGY OF GEOGRAPHIC ATROPHY SECONDARY TO AGE-RELATED MACULAR DEGENERATION AND THE COMPLEMENT PATHWAY AS A THERAPEUTIC TARGET

Boyer, David S. MD*; Schmidt-Erfurth, Ursula MD; van Lookeren Campagne, Menno PhD; Henry, Erin C. PhD; Brittain, Christopher MBBS§

doi: 10.1097/IAE.0000000000001392
Review

Purpose: Geographic atrophy (GA) is an advanced, vision-threatening form of age-related macular degeneration (AMD) affecting approximately five million individuals worldwide. To date, there are no approved therapeutics for GA treatment; however, several are in clinical trials. This review focuses on the pathophysiology of GA, particularly the role of complement cascade dysregulation and emerging therapies targeting the complement cascade.

Methods: Primary literature search on PubMed for GA, complement cascade in age-related macular degeneration. ClinicalTrials.gov was searched for natural history studies in GA and clinical trials of drugs targeting the complement cascade for GA.

Results: Cumulative damage to the retina by aging, environmental stress, and other factors triggers inflammation via multiple pathways, including the complement cascade. When regulatory components in these pathways are compromised, as with several GA-linked genetic risk factors in the complement cascade, chronic inflammation can ultimately lead to the retinal cell death characteristic of GA. Complement inhibition has been identified as a key candidate for therapeutic intervention, and drugs targeting the complement pathway are currently in clinical trials.

Conclusion: The complement cascade is a strategic target for GA therapy. Further research, including on natural history and genetics, is crucial to expand the understanding of GA pathophysiology and identify effective therapeutic targets.

Geographic atrophy is an advanced form of age-related macular degeneration that can significantly impact visual function, but has no approved treatment. This review focuses on the pathophysiology of geographic atrophy, particularly the role of complement cascade dysregulation and emerging therapies targeting the complement cascade.

*Retina Vitreous Associates, Los Angeles, California;

Department of Ophthalmology and Optometry, Medical University of Vienna, Vienna, Austria;

Genentech, Inc, South San Francisco, California; and

§F. Hoffmann-La Roche Ltd, Basel, Switzerland.

Reprint requests: David S. Boyer, MD, Retina Vitreous Associates, Medical Group, 1127 Wilshire Boulevard, Suite 1620, Los Angeles, CA 90017; e-mail: vitdoc@aol.com

Third-party writing assistance was provided by Kathryn H. Condon, PhD, CMPP, of Envision Scientific Solutions and funded by Genentech, Inc.

D. S. Boyer: Consultant for Allergan, Alcon, Aerpio, Allegro, Bausch & Lomb, Bayer, Genentech, Roche, Regeneron, Ohr, Optovue, Santen, Novartis. U. Schmidt-Erfurth: Consultant for Bayer, Alcon, Novartis, Boehringer. M. van Lookeren Campagne and E. C. Henry are employees of Genentech, Inc. C. Brittain is an employee of F. Hoffmann-La Roche Ltd.

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Geographic atrophy (GA) is an advanced, vision-threatening form of age-related macular degeneration (AMD). This degenerative disease occurs with progressive loss of areas of the retinal pigment epithelium (RPE), photoreceptors, and underlying choriocapillaris.1 Loss of visual function because of GA is considered irreversible and usually bilateral, with half of patients developing GA in both eyes within seven years of the initial GA diagnosis.2

An estimated 973,000 people in the United States3 and approximately 5 million globally4,5 have GA in at least one eye. In the United Kingdom, GA is estimated to account for 26% of legal blindness.6,7 The incidence of advanced AMD increases exponentially with age, with the two forms of advanced AMD, GA and neovascular AMD, occurring with roughly equal prevalence.4,5,8 As the population ages, the prevalence of advanced AMD is expected to rise from 9.64 million to 11.26 million in 2020 and 18.57 million in 2040.5

Currently, there is no efficient prevention, individual risk estimation, or reliable prognostic evaluation available, and, most importantly, there are no therapeutics approved for the treatment of GA. However, a number of drugs are in clinical trials. In particular, several of these target the complement cascade, a part of the innate immune system that can cause inflammation and cell death. Dysregulation of the complement cascade has been implicated in multiple chronic progressive diseases, including GA,9,10 and complement inhibition has been identified as a likely candidate for efficient therapeutic intervention. This review will focus on the pathophysiology of GA, particularly the role of complement cascade dysregulation and emerging therapies targeting the complement cascade.

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Pathology of Geographic Atrophy

Early stages of AMD are characterized by the presence and accumulation of drusen, extracellular deposits of cellular debris including protein and lipid aggregates, which appear clinically as yellowish dots at the posterior pole of the retina. Two large epidemiologic studies, Age-Related Eye Disease Study (AREDS) and Beaver Dam Eye Study, demonstrated that appearance and growth of drusen deposits are prognostic for GA. Eyes with multiple large drusen (>125 µm) are significantly more likely to develop GA than eyes with small drusen (<63 µm) (15-year odds ratio [OR], 14.5, 95% confidence interval [CI], 5.9–35.711; 10-year rate in 75 to 80 year olds, 26%12). Similarly, eyes with soft indistinct drusen (15-year OR, 14.6, 95% CI, 6.8–31.1) or pigmentary abnormalities (15-year OR, 15.2, 95% CI, 7.3–31.6) are also more likely to develop GA.11

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Imaging of Geographic Atrophy

Geographic atrophy can be imaged and monitored by multiple modalities, such as color fundus photography (CFP), fluorescein angiography (FA), fundus autofluorescence (FAF), red-free (RF) imaging, near infrared-wavelength FAF (NIR-FAF), and spectral-domain optical coherence tomography (SD-OCT) (Figure 1).13 Atrophic patches appear as generally well-demarcated areas, and choroidal vessels are increasingly visible in the absence of the overlaying RPE. Each imaging modality provides insight into different aspects of GA pathology and progression.

Fig. 1

Fig. 1

Fundus autofluorescence imaging detects the autofluorescence of lipofuscin, thought to be incompletely degraded photoreceptor outer segments and visual cycle by-products such as A2E, which accumulate within RPE cells.14,15 Complete absence of lipofuscin, appearing as dark, hypofluorescent regions, is used as a quantitative assessment of RPE cell death and an indirect measure of overlying photoreceptor loss.

Recent advances in high-resolution imaging techniques such as SD-OCT and adaptive optics scanning laser ophthalmoscopy (AOSLO) have allowed improved imaging of retinal features.16,17 Adaptive optics scanning laser ophthalmoscopy technology provides sufficient resolution to enable en face visualization of individual cone photoreceptors. Using this technique, structural changes in cone photoreceptors have been reported over drusen and at GA lesion boundaries.17 The cross-sectional images produced by SD-OCT allow detailed imaging of all retinal layers, including photoreceptors, RPE, and choroid. Comparative studies have shown generally high agreement between SD-OCT and FAF.16 However, SD-OCT offers clear advantages compared with en-face FAF as it allows a three-dimensional visualization of neurosensory atrophy, RPE alteration at the junctional border of GA lesions and central RPE loss, and choriocapillary thinning and choroidal enhancement because of increased light transmission resulting from melanocyte loss.18,19 In particular, foveal integrity is only reliably detected by SD-OCT and correlates tightly with visual function.19 The presence, number, and change in axial distribution of discrete hyperreflective loci on SD-OCT, thought to represent RPE cell migration from their native location in the outer retinal layer to ectopic locations in the inner retinal layers, have been recognized as a potential biomarker for progression from intermediate AMD to GA.20 Analysis of retinal layers on SD-OCT has led to the description of an early form of drusen-associated atrophy, termed “nascent GA,” which is associated with the subsidence of the outer plexiform layer and inner nuclear layer.21 Further analysis of these pathognomonic features of GA by SD-OCT may provide additional insight into the pathophysiology of GA.

Polarization-sensitive OCT (PS-OCT) is an advanced SD-OCT modality that selectively visualizes the RPE through the intrinsic polarization of incident light by RPE-specific melanocytes. This allows for the detection of discrete RPE changes in early AMD as well as a precise qualitative and quantitative evaluation of advanced GA lesions.22,23 For example, PS-OCT has identified additional features of drusen morphology, such as nonhomogeneity,24 which may correlate with RPE degeneration.25

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Patterns of Disease Progression

Geographic atrophy is a progressive disease,26,27 and progression rates can vary depending on baseline size,2,26–30 atrophy location,31 and the patterns of autofluorescence surrounding atrophic areas on FAF images (Figure 2).28 Geographic atrophy lesions are often multifocal, and the total atrophic area in eyes with multifocal lesions has been reported to grow faster than in eyes with unifocal lesions.30,32,33 With the exception of very large and very small GA lesions, atrophic patches generally grow linearly over time2,34; a square root transformation can be used to normalize enlargement rates to account for differences in baseline size in a population.30,34

Fig. 2

Fig. 2

Geographic atrophy is often bilateral; in AREDS, the cumulative probability of having bilateral GA at first GA development was 0.07 (95% CI, 0.05–0.09), increasing to 0.62 (95% CI, 0.52–0.72) at 10 years with a median time of 7 years (95% CI, 6.0–10.0 years) to progression to bilateral GA.2 In addition, there is a high degree of concordance between eyes with regard to GA incidence, progression, and area.2,27,35,36

The foveal-sparing growth patterns of GA suggest that the fovea is less susceptible to atrophy than extrafoveal regions.31,37 In an early study, foveal sparing was reported until about >1 disc area (DA) of atrophy was present,37 and recently, it was demonstrated that GA progression toward the periphery is 2.8 times faster than toward the fovea.38 This can result in a horseshoe- or ring-shaped area of GA surrounding the fovea.39 Based on this characteristic location and growth pattern, it is hypothesized that rods are preferentially, though not exclusively, affected over cones in GA; this is also supported by compromised scotopic retinal sensitivity in eyes with AMD.40,41

In AREDS GA progressed from noncentral to central GA, defined as definite GA involving the center point of the fovea, in a median 2.5 years following any GA diagnosis, with 35% of participants presenting with center-involved GA at the initial diagnosis.2 In the Beaver Dam Eye Study, 50% presented with foveal involvement at first diagnosis.32

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Functional Impact of Progression of Geographic Atrophy

Only a few studies have evaluated long-term GA progression patterns (≥2 years),2,27,32,42 and data on visual function in particular are sparse. Three natural history studies reported losses of more than three Early Treatment Diabetic Retinopathy Study (ETDRS) lines in best-corrected visual acuity (BCVA)2 in 439 or 52,32 years; however, some central GA was already present in all2 or many11,39 of these eyes at the baseline measurement. As GA impacts the visual field to varying degrees depending on lesion location, tasks dependent on full-field central vision such as reading39,43–45 may be impaired to a greater extent than is apparent from BCVA. Maximum reading rate correlates with the size of the atrophic area44 and is a significant risk factor for subsequent visual acuity loss.39,45

Patients with early/intermediate AMD and GA experience increased visual impairment under low-light conditions. Deficits in visual acuity under reduced illumination (low luminance visual acuity; LLVA) may precede and be larger than losses in BCVA under normal illumination.39,45–47 The low-luminance deficit, or difference between LLVA and BCVA, is potentially predictive of subsequent visual acuity loss and GA progression.39,48 Conversely, patients with early AMD who report better night vision are less likely to develop GA.49 Quantitative analysis of dark adaptation has shown that dark adaptometry has high sensitivity and specificity for diagnosing AMD, which may be of clinical utility considering the short time required to perform the measurement (≤6.5 minutes).50 While the utility of this technique in the assessment of GA lesion progression remains to be studied, impairments in dark adaptation have been shown to be positively correlated with age, worse visual acuity, presence of reticular pseudodrusen, AMD severity, and subfoveal choroidal thinning.51

Microperimetry, which maps a patient's threshold light sensitivity onto the retina, provides a link between retinal function and anatomy; areas where the patient cannot detect light of the highest testable intensity indicate scotomas. Decreases in retinal sensitivity over time correlate with GA progression,52 morphological alterations on SD-OCT,53 increased fluorescence on FAF,54 and decreases in LLVA.47 Similar to LLVA, functional mapping by microperimetry reveals greater visual deficits under scotopic conditions in early stages of AMD, and absolute defects once GA has become manifest. Microperimetry may also detect more widespread decreases in retinal sensitivity in the perilesional areas.52

In later stages of GA, large central scotomas develop, effectively resulting in legal blindness. Upon progression of GA to the fovea, central fixation is lost and an extrafoveal preferred fixation locus may develop.43

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Pathogenesis of Geographic Atrophy

The pathogenesis of GA is multifactorial and is generally thought to be triggered by intrinsic and extrinsic stressors of the poorly regenerative RPE, particularly oxidative stress caused by the high metabolic demand of photoreceptors, photo-oxidation, and environmental stressors such as cigarette smoke. With aging, the damage caused by these stressors accumulates, resulting in the appearance of drusen (extracellular) and lipofuscin (intracellular) deposits.55 Components of drusen (cellular debris, lipids, lipoproteins, amyloid deposits) and lipofuscin (by-products of photoreceptor outer-segment degradation, A2E), as well as other products of oxidative stress such as advanced glycation end products, are thought to trigger inflammation via multiple pathways, such as the complement cascade and the NLRP3 inflammasome. When the regulatory components in these pathways are compromised, as is the case with several GA-linked genetic risk factors in the complement cascade, this inflammation can ultimately lead to the retinal cell death characteristic of GA.

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The Complement Cascade

A leading contributor to the pathogenesis of AMD is inappropriate complement cascade-mediated inflammation.10,56 The complement cascade is primarily involved in the detection and removal of foreign pathogens such as bacteria.9,57–62 Involving more than 30 known cell-associated and systemically circulating proteins, activation of the complement cascade can lead to inflammation, opsonization, phagocytosis, and cell death through the formation of the membrane attack complex (MAC).

The complement cascade consists of three separate pathways, each activated by different factors: antigen–antibody complexes (classical complement pathway), polysaccharides on microorganisms (lectin complement pathway), and pathogen cell surfaces (alternative complement pathway) (Figure 3). In addition, the alternative complement pathway continuously undergoes spontaneous low-level activation. These different pathways converge with the cleavage of complement factor C3 into C3a and C3b, which induce inflammation and label (opsonize) cells for phagocytosis, respectively. On host cells, endogenous factors shut down the complement cascade. On pathogens, the complement cascade continues with the cleavage of complement factor C5, which triggers cell death via phagocytosis, inflammation, and ultimately MAC activation. Of note, genetic variants associated with GA risk strongly implicate the alternative complement pathway in disease pathogenesis.63,64 An overview of the complement cascade and a summary of key evidence supporting its role in GA pathogenesis follows.

Fig. 3

Fig. 3

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Initiation

The three complement pathways are initiated by different factors, each resulting in the cleavage of complement factor C3.

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Classical

The classical complement pathway is activated when the C1 complex binds specific antigen–antibody complexes, often immunoglobulin M (IgM), IgG3, or IgG1. This induces a conformational change in the C1 complex, allowing it to cleave C4 and C2 to generate the C4bC2b complex. C4bC2b acts as the C3 convertase of the classical pathway, cleaving C3 into C3a and C3b.

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Lectin

The lectin complement pathway is activated when mannose-binding lectin (MBL) binds mannose-containing polysaccharides on microorganisms, initiating the cleavage of C4 and C2 by the MBL–MBL-associated serine protease (MASP) complex. As in the classical pathway, the C4bC2b complex forms the C3 convertase of the lectin pathway.

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Alternative

The oldest evolutionary signaling pathway of the three, the alternative complement pathway acts both independently of, and as an amplification loop for, the classical and lectin pathways.60 The alternative complement pathway undergoes low-level self-activation through the slow, spontaneous hydrolysis of C3 termed “tickover.” Once hydrolyzed, C3(H2O) binds complement factor B (CFB), which is subsequently cleaved by complement factor D (CFD) into C3(H2O)Bb, forming the initial C3 convertase of the alternative complement pathway.

Complement factor D is the rate-limiting enzyme in alternative complement pathway activation.65 Increasing concentrations of CFD, which circulates only in an active form, can directly enhance complement cascade activity.66

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Amplification via the alternative complement pathway

Cleavage of C3 by any of the C3 convertases exposes a thioester group on C3b, through which C3b can covalently bind to the surface of pathogen or host cells via hydroxyl groups on carbohydrates.67 C3b then binds to CFB, which is cleaved by CFD into Bb and Ba. This forms the primary C3 convertase of the alterative pathway, C3bBb, which continues to cleave C3 and thus amplifies complement cascade activation. In this manner, amplification via the alternative complement pathway may account for more than 80% of total complement activation.68,69

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Host cells: termination of the complement cascade

On host cells, endogenous factors including regulatory proteins inactivate the C3 convertases, terminating the complement reaction. C3b and C4b are bound by endogenous regulators of complement activation such as complement receptor 1 (CR1), decay accelerating factor (DAF/CD55), complement Factor H (CFH; primarily C3b), C4-binding protein (C4BP; primarily C4b), and membrane cofactor protein (MCP/CD46), which displace Bb or C2b (DAF, CR1) and/or act as cofactors for complement factor I (CFI)-mediated cleavage and inactivation of C3b and C4b.

Rapid inactivation of the complement cascade is critical to localize the reaction to pathogens and prevent complement attack of host cells. Notably, CFI is a rate-limiting enzyme of complement termination; increasing CFI concentration by just 25% can effectively shut down alternative complement pathway activation in in vitro experiments.60,70 This implies that a small change in CFI activity or abundance may have significant effects on complement cascade activity.

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Pathogens: stabilization and amplification of the complement cascade

On pathogens, the C3 convertase complexes are stabilized on the cell surface, while the absence of endogenous regulatory proteins prevents inactivation. In the alternative complement pathway, properdin (complement factor P) binds to and stabilizes C3bBb on the cell surface.

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Formation of the C5 convertase, inflammation, phagocytosis, and the membrane attack complex

The classical, lectin, and alternative complement pathways converge with the cleavage of C3 into C3a and C3b and the subsequent formation of the C5 convertase complexes of C4bC2bC3b (classical, lectin pathways) or C3bC3bBb (alternative complement pathway). These C5 convertase complexes cleave C5 into C5a and C5b, initiating the final steps of the complement cascade.

Inflammation is initiated by C3a, C4a, and C5a, which induce smooth muscle contraction, increase vascular permeability, and control migration of neutrophils and monocytes. C3a and C5a activate mast cells to release histamine, tumor necrosis factor (TNF)-α, and other inflammatory factors, further recruiting antibody, complement, and phagocytic cells to the site of complement activation.

Pathogen cell death is ultimately accomplished by the MAC, a complex of C5b, C6, C7, C8, and the C9 polymer, initiated by C5b. The MAC creates pores in the pathogen cell surface, destroying the lipid bilayer, disrupting proton gradients, and allowing penetration of enzymes, resulting in pathogen or cell destruction.

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Role of Complement in Health and Disease

Although the complement cascade is traditionally considered part of the immune system, and therefore charged with protecting against foreign pathogens, complement activity also has important roles in maintaining healthy tissue. Clearance of apoptotic cells is facilitated by the complement pathway, which opsonizes the cells for removal via phagocytosis.62 Apoptotic cells shed membrane-bound complement regulators such as MCP/CD46 and CD59,71 while the presence of circulating complement regulators, for example, CFH, prevents the reaction from escalating and affecting nearby cells.61 Additional nonimmunological physiological roles for complement activity include neuronal synapse remodeling,72,73 lipid metabolism,74 and bone remodeling.75

When the function or expression of complement regulators is compromised, otherwise healthy cells can become susceptible to complement attack (Figure 4). This loss of appropriate complement regulation is thought to underlie a number of diseases, including AMD.9 As discussed below, genetic variations in complement proteins, such as in C3, CFH, and CFI, decrease complement inactivation, thus rendering cells vulnerable to inappropriate complement attack.

Fig. 4

Fig. 4

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Evidence for Complement Cascade Dysfunction in Geographic Atrophy

The case for complement cascade dysfunction in AMD is supported by three key lines of evidence. Landmark genome-wide association studies (GWAS) identified AMD-associated variants in complement factor genes, particularly those such as CFH that promote alternative complement pathway termination on host cells.63 In addition, patients with GA exhibit alterations in complement cascade components both systemically and locally within the eye. Finally, these observations are supported by preclinical research in vitro and in mice, which have demonstrated that complement dysfunction is associated with GA-like pathology.76 Evidence supporting the role of complement cascade dysfunction and the pathogenesis of GA is discussed in detail below.

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Genetic evidence for complement cascade dysfunction in geographic atrophy

Development of advanced AMD is strongly influenced by genetics. Early genome-wide and targeted sequencing studies identified a common variant in the CFH gene associated with AMD risk (CFH Y402H)77–80 estimated to account for nearly half of AMD risk.78–80 More recently, a meta-analysis and validation sequencing of GWAS data by the AMD Consortium, which evaluated >17,100 advanced AMD cases and >60,000 controls for common AMD risk variants, identified 19 single nucleotide polymorphisms (SNPs), of which four are contained within complement cascade genes (CFH, CFI, C3, C2/CFB).81 Other identified SNPs are associated with genes involved in lipid metabolism, extracellular matrix remodeling, and angiogenesis.81 In addition, individually rare coding variants have been identified in CFI, CFH, C3, and C9.82–87

Many of these variants are predicted to increase activation or decrease inactivation of the complement cascade, thereby altering the physiological balance toward increased inflammatory processes, supplying perhaps the strongest evidence for the involvement of complement in AMD. Each of the CFH Y402H, CFH R1210C, and C3 K155Q variants are predicted to reduce the interaction between CFH and C3b, thus diminishing complement cascade inactivation and potentially increasing feedback amplification of the alternative complement pathway.79,82,84,87–89 Of note, the rare, highly penetrant CFH R1210C variant is associated with a 6-year earlier onset of AMD83 and is also a risk allele for rare glomerulopathies linked to inappropriate alternative complement pathway regulation.90,91 Patients with these glomerulopathies also display phenotypic changes consistent with early AMD.90 Similarly, many of the rare CFI risk variants are predicted to be damaging to CFI function and thus decrease complement cascade inactivation.84,85,92 The rare CFI G119R variant, which reduces CFI expression and C3b degradation, confers a particularly high risk of AMD (OR, 22.20; 95% CI, 2.98–164.49).85

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Physiological evidence for complement cascade dysfunction in geographic atrophy

In addition to the strong genetic association, complement cascade dysfunction has been detected both systemically and in human donor eyes of patients with advanced AMD, including GA. Complement activation products, such as C3d (a breakdown product of C3b after cleavage by CFI), C3a, Ba, Bb, and C5a, are elevated in plasma of patients with AMD93 and GA94; alterations in levels of plasma CFD93,95 and CFI92,96 have also been reported. Drusen derived from human donor eyes contain complement factors C3,97,98 C5,98–100 CFH,80,101 and activated MAC.99,100 Transcriptome profiling of AMD versus control retinal tissue demonstrated upregulation of complement pathway genes.102 Bruch's membrane/choriocapillaris extracts from advanced AMD eyes contained elevated CFB, C3, C3a, and CFD levels compared with eyes lacking macular drusen,97 and MAC is elevated in the choriocapillaris of eyes with the high-risk CFH allele.103,104 Reductions in MCP/CD46, a cofactor for CFI-mediated cleavage of C3b and C4b, were observed in early AMD and GA donor eyes, preceding atrophy and correlating with disease severity.105,106

Evidence of systemic complement cascade dysfunction has also been found in patients with AMD-associated variants in complement factor genes. The GA-associated CFH variant has been reported to be associated with elevated choroidal101 or systemic107–109 markers of inflammation, higher levels of oxidated phospholipids in plasma,110 and increased presence of complement activation products.93,103,111 Similarly, individuals with advanced AMD and rare CFI variants had significantly lower serum CFI levels compared with those without AMD; lower CFI serum levels were associated with a greater risk of advanced AMD among those with (OR, 13.6; P = 1.6 × 10−4) and without (OR, 19.0; P = 1.1 × 10−5) a rare CFI variant.92

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Preclinical research on complement dysfunction in geographic atrophy

A number of preclinical studies provide proof-of-concept support and mechanistic insight into complement dysfunction and GA pathogenesis.

Studies in mouse models of complement dysregulation support a causal role for complement in retinal pathology.112 In the absence of a specific environmental or immune challenge, CFH deficiency in mice is sufficient to cause age-related decreased visual acuity, reduced photoreceptor activity under scotopic conditions, altered retinal autofluorescence, and increased C3 deposition in the retina.113 The phenotype can be rescued by expression of human CFH. 114 Transgenic mice expressing the human CFH Y402H risk variant, which may better mimic complement dysregulation in human disease, develop an AMD-like pathology including subretinal drusen-like deposits, accumulation of subretinal macrophage/microglia, basal laminar deposits, and increased numbers of lipofuscin granules.115 In addition, C3 overexpression leads to retinal pathology,116 while conversely, CFD-deficient mice are protected against photoreceptor loss from chronic light exposure compared with wild-type mice.117 Recently, alternative complement pathway activation was implicated in photoreceptor cell death following retinal detachment,118 further emphasizing a role for this pathway in photoreceptor degeneration.

It is believed that environmental risk factors and oxidative stress, coupled with genetic risk factors, can trigger complement-induced retinal cell death. In a proof-of-concept study, an immune response to carboxyethylpyrrol (CEP), an oxidation fragment of the polyunsaturated fatty acid docosahexaenoic acid (DHA) abundant in the outer retina, was sufficient to cause complement C3d deposition in Bruch's membrane and AMD-like lesions in mice.76 Photo-oxidation products of A2E, a component of lipofuscin, can trigger CFB-dependent complement activation in RPE cells.119,120 In mice, chronic exposure to cigarette smoke led to reduced photoreceptor function and complement C3d deposition at the RPE/Bruch's membrane and choroid, while CFB-deficient mice were protected against similar retinal damage.121

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NLRP3 Inflammasome

Other pathways, such as inflammasome activation, have also been implicated in GA pathogenesis. The NLRP3 inflammasome is a multiprotein scaffold consisting mainly of NLRP3, the adaptor molecule ASC, and caspase-1. Activation of the NLRP3 inflammasome can lead to caspase-mediated processing of the cytokines interleukin (IL)-1β and IL-18, key mediators of innate and adaptive immunity, and cleavage of gasdermin D that drives pyroptosis, a lytic type of cell death.122 While inflammasome activation has been associated with loss of RPE cells,123–125 the molecular mechanism of inflammasome-mediated RPE cell death has yet to be defined. Research continues in effort to determine pathways that trigger the NLRP3 inflammasome either via activation (stimulation of inflammasome complex signaling) or priming (upregulation of inflammasome-related genes). One trigger appears to be accumulation of RNA. A GA-like model of RPE degeneration in mice can be initiated by downregulation of the RNA processor enzyme DICER1, which leads to RNA accumulation and cell death via NLRP3 inflammasome activation.123,126 Decreased DICER1 expression and the resulting accumulation of RNA have been found in human donor eyes with GA.126

Drusen components also trigger the inflammasome. It has been demonstrated that when drusen are excised from donor eyes and then added in vitro to macrophages and dendritic cells, the ASC inflammasome component becomes activated and IL-1β/IL-18 production occurs.125 Similarly, when individual drusen components such as A2E (the major fluorophore of lipofuscin) are added in vitro to cultured RPE cells, these cells then secrete IL-1β via inflammasome activation in response to the A2E insult.127 In a mouse model, intravitreal injection of the drusen component amyloid-β led to genetic upregulation of inflammasome components in the neuroretina and corresponding increased levels of IL-1β and IL-18.128

C1q is one of several complement system factors found in drusen, and the addition of C1q to macrophages induces in vitro inflammasome component activation and production of IL-1β.125 Exogenous administration of other complement components such as C3a,129 C5a,130 and MAC131,132 also activates the NLRP3 inflammasome. Thus, current in vitro studies indicate that activation of the complement system has the downstream effect of inflammasome-mediated cytokine signaling through IL-1β and IL-18. The interaction between complement and inflammasome pathways is an emerging area of research, and as in vitro findings are further explored through in vivo studies, the roles these two systems play in the pathophysiology of GA will be more clearly understood.

The overall role of the inflammasome on neovascular AMD pathogenesis is a subject of active debate.133,134 Inflammasome-mediated production of IL-18 has been shown to protect against neovascularization,125,133,135 and intravitreal administration of IL-18 is being explored as a therapy for neovascular AMD.133 Additional mechanistic studies are required to shed light on this controversy.

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Natural History Studies in Geographic Atrophy

Studies on the natural history of GA and age-related macular degeneration have provided much valuable information regarding the progression, epidemiology, and environmental risk factors of GA.2,11,12,27,28,32,136–138 However, there are still gaps in our understanding of the natural history of the disease, which ongoing and upcoming studies aim to address. Two studies, SIGHT (NCT02332343) and DSGA (NCT02051998) will investigate differential patterns of atrophy progression in the retina, namely foveal sparing and directional spread of atrophic areas, respectively. Three other studies will study GA using different types of retinal imaging, namely FAF (NCT00393692), OCT (NCT01712841), and AOSLO (NCT01866371).

Proxima, a large natural history study program with a global enrollment target of 560 patients, is evaluating the relationship between GA progression and visual function outcomes as well as the prognostic nature of the CFI biomarker. Proxima consists of two cohorts: Proxima A (NCT02479386), designed to have a population similar to the Phase 3 Chroma and Spectri trials (see below), will include patients with bilateral GA; while Proxima B (NCT02399072) will include a broader cohort of patients, that is, those generally excluded from Phase 3 trials (unilateral GA, GA with choroidal neovascularization [CNV] in the fellow eye). Patients will be followed every 6 months, and assessed outcomes will be similar to those of Chroma and Spectri.

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Clinical Development of Potential Pharmacotherapies

Although no drugs are currently available in clinical practice for the treatment of GA, a number of therapeutics are at various stages of clinical development. Among these are six drugs that target the complement cascade (Table 1), including three targeting C5, one targeting C3, and one targeting the alternative complement pathway (Figure 5). To date, limited information is available for LFG316 (anti-C5; Novartis International AG, Basel, Switzerland), Zimura (C5 inhibitor; Ophthotech Corporation, New York, NY), and CLG561 (anti-properdin; Novartis and Alcon Inc, Hünenberg, Switzerland). APL-2 (C3 inhibitor; Apellis Pharmaceuticals, Crestwood, KY), eculizumab (anti-C5; Alexion Pharmaceuticals, Inc, Cheshire, CT), and lampalizumab (anti-CFD; Genentech, Inc, South San Francisco, CA and F. Hoffmann-La Roche AG, Basel, Switzerland), which have completed Phase 2 trials, are discussed below.

Table 1

Table 1

Fig. 5

Fig. 5

Beyond the complement cascade, therapies are in development to target other GA-implicated pathways such as anti-inflammatory agents, amyloid-β scavengers, choroidal perfusion enhancers, serotonin receptor agonists, and stem cell therapies; discussion of these agents can be found in other recent reviews.1,139,140 Other approaches in preclinical development include nucleoside reverse transcriptase inhibitors (NRTIs), which are already approved for the treatment of HIV infection,141 and a modulator of the innate inflammatory profile (TMi-18; Translatum Medicus Inc, Toronto, ON, Canada).142

APL-2 (POT-4/AL-78898A, Apellis Pharmaceuticals) is an intravitreally administered peptide inhibitor of C3. Phase 2 trials of POT-4/AL-78898A were terminated before primary endpoint, and therefore no efficacy data are currently available (NCT01603043). APL-2 is a modified version of POT-4 designed to have a longer half-life.143 The Phase 2 FILLY trial (NCT02503332) of APL-2 in patients with GA is currently ongoing.

Eculizumab (Soliris, Alexion Pharmaceuticals, Inc) is an intravenously (IV) administered humanized monoclonal antibody targeting C5, approved by the United States Food and Drug Administration (FDA) and European Medicines Agency (EMA) for the treatment of two rare genetic deficiencies of complement inhibition, atypical hemolytic uremic syndrome and paroxysmal nocturnal hemoglobinuria.144 Eculizumab binds to C5, inhibiting its cleavage into C5a and C5b, thereby preventing MAC formation.

The Phase 2 COMPLETE trial (NCT00935883) evaluated eculizumab in 30 eyes of 30 patients with eligible GA lesion area from 1.25 to 18 mm2 who received high-dose eculizumab (n = 10; IV 900 mg for 4 weeks followed by 1,200 mg every 2 weeks until week 24), low-dose eculizumab (n = 10; IV 600 mg for 4 weeks followed by 900 mg every 2 weeks until week 24), or placebo (n = 10) over 24 weeks.48 The primary efficacy endpoint was change in GA area assessed by SD-OCT at 26 weeks, with additional follow-up at 52 weeks. However, GA enlargement from baseline was similar at each time point between eculizumab and placebo groups (change from baseline of mean square root of GA area ± standard deviation [SD]: 26 weeks, 0.19 ± 0.12 vs. 0.18 ± 0.15 mm, respectively, P = 0.96; 52 weeks, 0.37 ± 0.21 vs. 0.37 ± 0.22 mm, respectively; P = 0.93). No drug-related adverse events (AEs) were reported in COMPLETE patients through 12 months.

While the study was powered to only detect at least a 55% difference in GA progression, the lack of any trend toward efficacy with eculizumab led the study authors to conclude that “after 26 weeks we can say definitively that the treatment failed to meet this endpoint.” Eculizumab for GA is no longer listed among Alexion's pipeline therapeutics.145,146 At this time, it is not clear whether the failure of eculizumab was because of the choice of C5 as a target, insufficient ocular bioavailability in systemic (vs. intravitreal) administration, study design, or other factors.48 For example, inhibiting C5 does not block the actions of C3 (e.g., C3a-induced inflammation and C3b/iC3b-mediated opsonophagocytosis).

Lampalizumab (FCFD4514S/anti-factor D, Genentech, Inc and F. Hoffmann-La Roche AG) is an intravitreally administered antigen-binding fragment (Fab) of a humanized monoclonal antibody targeting CFD. Lampalizumab binds to CFD, preventing CFD-mediated activation of C3bBb and effectively terminating activation and amplification of the alternative complement pathway.147

As discussed above, CFD is the rate-limiting enzyme of the alternative complement pathway and is present in low serum concentrations relative to other complement factor proteins.93,96 Inhibiting CFD decreases, but does not eliminate, classical and lectin-activated complement initiation.68,69 Intravitreal clinically relevant doses were demonstrated to have minimal systemic inhibition of the alternative complement pathway in pharmacokinetic studies in monkeys148,149 and in subjects participating in the Phase 1 and Phase 2 lampalizumab trials (NCT00973011; NCT01229215).150,151 The low levels of lampalizumab in systemic circulation resulting from intravitreal administration are not expected to affect systemic alternative complement pathway activity.148

The MAHALO Phase 2 study (NCT01229215) evaluated lampalizumab in patients with GA secondary to AMD and the results have been submitted for publication (Yaspan et al). Confirmatory Phase 3 trials Chroma (NCT02247479) and Spectri (NCT02247531) are ongoing. Chroma and Spectri are identically designed double-masked, multicenter, randomized, sham injection-controlled trials enrolling 936 participants each across more than 20 countries. Each study arm will contain patients positive and negative for the CFI biomarker. Patients are being randomized 2:1:2:1 to 10 mg lampalizumab every 4 weeks, sham injection every 4 weeks, 10 mg lampalizumab every 6 weeks, and sham injection every 6 weeks. The primary efficacy endpoint is the mean change in GA area at 1 year, and the overall study duration is 2 years. Additional visual function secondary endpoints include reading speed, Patient Reported Outcome (PRO) Visual Function Questionnaire (VFQ)-25, microperimetry, LLVA, and BCVA.

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Conclusion

Dysregulation of the complement cascade has emerged as a key contributor to the pathophysiology of GA, supported by a number of genetic, histological, and preclinical studies. With several Phase 2 and 3 clinical trials already in progress, there is at present a significant impetus toward identifying complement targets that may prove effective at limiting retinal cell death in patients with GA. Continued research, including studies on the initial development of GA, GA lesion progression, genetics, and the contribution of each to subsequent visual function decline, is crucial to further our understanding of GA pathophysiology and to identify additional potential therapeutic targets.

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References

1. Holz FG, Strauss EC, Schmitz-Valckenberg S, Van Lookeren Campagne M. Geographic atrophy: clinical features and potential therapeutic approaches. Ophthalmology 2014;121:1079–1091.
2. Lindblad AS, Lloyd PC, Clemons TE, et al. Change in area of geographic atrophy in the Age-Related Eye Disease Study: AREDS report number 26. Arch Ophthalmol 2009;127:1168–1174.
3. Friedman DS, O'Colmain BJ, Munoz B, et al. Prevalence of age-related macular degeneration in the United States. Arch Ophthalmol 2004;122:564–572.
4. Rudnicka AR, Jarrar Z, Wormald R, et al. Age and gender variations in age-related macular degeneration prevalence in populations of European ancestry: a meta-analysis. Ophthalmology 2012;119:571–580.
5. Wong WL, Su X, Li X, et al. Global prevalence of age-related macular degeneration and disease burden projection for 2020 and 2040: a systematic review and meta-analysis. Lancet Glob Health 2014;2:e106–116.
6. Definition of blindness given in: United Kingdom Department of Health. Certificate of vision impairment explanatory notes for consultant ophthalmologists and hospital eye clinic staff. 2013. Available at: https://www.gov.uk/government/uploads/system/uploads/attachment_data/file/213286/CVI-Explanatory-notes-in-DH-template.pdf. Accessed October 15, 2015.
7. Rees A, Zekite A, Bunce C, Patel PJ. How many people in England and Wales are registered partially sighted or blind because of age-related macular degeneration? Eye (Lond) 2014;28:832–837.
8. Ferris FL III, Wilkinson CP, Bird A, et al. Clinical classification of age-related macular degeneration. Ophthalmology 2013;120:844–851.
9. Wagner E, Frank MM. Therapeutic potential of complement modulation. Nat Rev Drug Discov 2010;9:43–56.
10. Ambati J, Atkinson JP, Gelfand BD. Immunology of age-related macular degeneration. Nat Rev Immunol 2013;13:438–451.
11. Klein R, Klein BE, Knudtson MD, et al. Fifteen-year cumulative incidence of age-related macular degeneration: the Beaver Dam Eye Study. Ophthalmology 2007;114:253–262.
12. Chew EY, Clemons TE, Agron E, et al. Ten-year follow-up of age-related macular degeneration in the Age-Related Eye Disease Study: AREDS report no. 36. JAMA Ophthalmol 2014;132:272–277.
13. Göbel AP, Fleckenstein M, Schmitz-Valckenberg S, et al. Imaging geographic atrophy in age-related macular degeneration. Ophthalmologica 2011;226:182–190.
14. Kennedy CJ, Rakoczy PE, Constable IJ. Lipofuscin of the retinal pigment epithelium: a review. Eye 1995;9:763–771.
15. Sparrow JR, Dowling JE, Bok D. Understanding RPE lipofuscin. Invest Ophthalmol Vis Sci 2013;54:8325–8326.
16. Simader C, Sayegh RG, Montuoro A, et al. A longitudinal comparison of spectral-domain optical coherence tomography and fundus autofluorescence in geographic atrophy. Am J Ophthalmol 2014;158:557–566. e551.
17. Zayit-Soudry S, Duncan JL, Syed R, et al. Cone structure imaged with adaptive optics scanning laser ophthalmoscopy in eyes with nonneovascular age-related macular degeneration. Invest Ophthalmol Vis Sci 2013;54:7498–7509.
18. Yehoshua Z, de Amorim Garcia Filho CA, Nunes RP, et al. Comparison of geographic atrophy growth rates using different imaging modalities in the COMPLETE study. Ophthalmic Surg Lasers Imaging Retina 2015;46:413–422.
19. Sayegh RG, Simader C, Scheschy U, et al. A systematic comparison of spectral-domain optical coherence tomography and fundus autofluorescence in patients with geographic atrophy. Ophthalmology 2011;118:1844–1851.
20. Christenbury JG, Folgar FA, O'Connell RV, et al. Progression of intermediate age-related macular degeneration with proliferation and inner retinal migration of hyperreflective foci. Ophthalmology 2013;120:1038–1045.
21. Wu Z, Luu CD, Ayton LN, et al. Optical coherence tomography-defined changes preceding the development of drusen-associated atrophy in age-related macular degeneration. Ophthalmology 2014;121:2415–2422.
22. Ahlers C, Götzinger E, Pircher M, et al. Imaging of the retinal pigment epithelium in age-related macular degeneration using polarization-sensitive optical coherence tomography. Invest Ophthalmol Vis Sci 2010;51:2149–2157.
23. Baumann B, Götzinger E, Pircher M, et al. Segmentation and quantification of retinal lesions in age-related macular degeneration using polarization-sensitive optical coherence tomography. J Biomed Opt 2010;15:061704.
24. Schlanitz FG, Sacu S, Baumann B, et al. Identification of drusen characteristics in age-related macular degeneration by polarization-sensitive optical coherence tomography. Am J Ophthalmol 2015;1602:335–344. e1.
25. Ouyang Y, Heussen FM, Hariri A, et al. Optical coherence tomography-based observation of the natural history of drusenoid lesion in eyes with dry age-related macular degeneration. Ophthalmology 2013;120:2656–2665.
26. Jeong YJ, Hong IH, Chung JK, et al. Predictors for the progression of geographic atrophy in patients with age-related macular degeneration: fundus autofluorescence study with modified fundus camera. Eye (Lond) 2014;28:209–218.
27. Sunness JS, Margalit E, Srikumaran D, et al. The long-term natural history of geographic atrophy from age-related macular degeneration: enlargement of atrophy and implications for interventional clinical trials. Ophthalmology 2007;114:271–277.
28. Holz FG, Bindewald-Wittich A, Fleckenstein M, et al. Progression of geographic atrophy and impact of fundus autofluorescence patterns in age-related macular degeneration. Am J Ophthalmol 2007;143:463–472.
29. Fleckenstein M, Schmitz-Valckenberg S, Adrion C, et al. Progression of age-related geographic atrophy: role of the fellow eye. Invest Ophthalmol Vis Sci 2011;52:6552–6557.
30. Yehoshua Z, Rosenfeld PJ, Gregori G, et al. Progression of geographic atrophy in age-related macular degeneration imaged with spectral domain optical coherence tomography. Ophthalmology 2011;118:679–686.
31. Mauschitz MM, Fonseca S, Chang P, et al. Topography of geographic atrophy in age-related macular degeneration. Invest Ophthalmol Vis Sci 2012;53:4932–4939.
32. Klein R, Meuer SM, Knudtson MD, Klein BE. The epidemiology of progression of pure geographic atrophy: the Beaver Dam Eye Study. Am J Ophthalmol 2008;146:692–699.
33. Xu L, Blonska AM, Pumariega NM, et al. Reticular macular disease is associated with multilobular geographic atrophy in age-related macular degeneration. Retina 2013;33:1850–1862.
34. Feuer WJ, Yehoshua Z, Gregori G, et al. Square root transformation of geographic atrophy area measurements to eliminate dependence of growth rates on baseline lesion measurements: a reanalysis of Age-Related Eye Disease Study report no. 26. JAMA Ophthalmol 2013;131:110–111.
35. Bellmann C, Jorzik J, Spital G, et al. Symmetry of bilateral lesions in geographic atrophy in patients with age-related macular degeneration. Arch Ophthalmol 2002;120:579–584.
36. Fleckenstein M, Adrion C, Schmitz-Valckenberg S, et al. Concordance of disease progression in bilateral geographic atrophy due to AMD. Invest Ophthalmol Vis Sci 2010;51:637–642.
37. Sarks JP, Sarks SH, Killingsworth MC. Evolution of geographic atrophy of the retinal pigment epithelium. Eye (Lond) 1988;2(Pt 5):552–577.
38. Lindner M, Boker A, Mauschitz MM, et al. Directional kinetics of geographic atrophy progression in age-related macular degeneration with foveal sparing. Ophthalmology 2015;122:1356–1365.
39. Sunness JS, Rubin GS, Zuckerbrod A, Applegate CA. Foveal-sparing scotomas in advanced dry age-related macular degeneration. J Vis Impair Blind 2008;102:600–610.
40. Owsley C, Jackson GR, White M, et al. Delays in rod-mediated dark adaptation in early age-related maculopathy. Ophthalmology 2001;108:1196–1202.
41. Owsley C, McGwin G Jr, Jackson GR, et al. Cone- and rod-mediated dark adaptation impairment in age-related maculopathy. Ophthalmology 2007;114:1728–1735.
42. Sunness JS, Rubin GS, Broman A, et al. Low luminance visual dysfunction as a predictor of subsequent visual acuity loss from geographic atrophy in age-related macular degeneration. Ophthalmology 2008;115:1480–1488. 1488 e1481–1482.
43. Sunness JS, Applegate CA. Long-term follow-up of fixation patterns in eyes with central scotomas from geographic atrophy that is associated with age-related macular degeneration. Am J Ophthalmol 2005;140:1085–1093.
44. Sunness JS, Applegate CA, Haselwood D, Rubin GS. Fixation patterns and reading rates in eyes with central scotomas from advanced atrophic age-related macular degeneration and Stargardt disease. Ophthalmology 1996;103:1458–1466.
45. Sunness JS, Rubin GS, Applegate CA, et al. Visual function abnormalities and prognosis in eyes with age-related geographic atrophy of the macula and good visual acuity. Ophthalmology 1997;104:1677–1691.
46. Puell MC, Barrio AR, Palomo-Alvarez C, et al. Impaired mesopic visual acuity in eyes with early age-related macular degeneration. Invest Ophthalmol Vis Sci 2012;53:7310–7314.
47. Wu Z, Ayton LN, Guymer RH, Luu CD. Low-luminance visual acuity and microperimetry in age-related macular degeneration. Ophthalmology 2014;121:1612–1619.
48. Yehoshua Z, de Amorim Garcia Filho CA, Nunes RP, et al. Systemic complement inhibition with eculizumab for geographic atrophy in age-related macular degeneration: the COMPLETE study. Ophthalmology 2014;121:693–701.
49. Ying GS, Maguire MG, Liu C, et al. Night vision symptoms and progression of age-related macular degeneration in the Complications of Age-Related Macular Degeneration Prevention Trial. Ophthalmology 2008;115:1876–1882.
50. Jackson GR, Scott IU, Kim IK, et al. Diagnostic sensitivity and specificity of dark adaptometry for detection of age-related macular degeneration. Invest Ophthalmol Vis Sci 2014;55:1427–1431.
51. Flamendorf J, Agron E, Wong WT, et al. Impairments in dark adaptation are associated with age-related macular degeneration severity and reticular pseudodrusen. Ophthalmology 2015;122:2053–2062.
52. Meleth AD, Mettu P, Agron E, et al. Changes in retinal sensitivity in geographic atrophy progression as measured by microperimetry. Invest Ophthalmol Vis Sci 2011;52:1119–1126.
53. Sayegh RG, Kiss CG, Simader C, et al. A systematic correlation of morphology and function using spectral domain optical coherence tomography and microperimetry in patients with geographic atrophy. Br J Ophthalmol 2014;98:1050–1055.
54. Schmitz-Valckenberg S, Bultmann S, Dreyhaupt J, et al. Fundus autofluorescence and fundus perimetry in the junctional zone of geographic atrophy in patients with age-related macular degeneration. Invest Ophthalmol Vis Sci 2004;45:4470–4476.
55. Ardeljan D, Chan CC. Aging is not a disease: distinguishing age-related macular degeneration from aging. Prog Retin Eye Res 2013;37:68–89.
56. Hageman GS, Luthert PJ, Victor Chong NH, et al. An integrated hypothesis that considers drusen as biomarkers of immune-mediated processes at the RPE-Bruch's membrane interface in aging and age-related macular degeneration. Prog Retin Eye Res 2001;20:705–732.
57. Janeway CJ, Travers P, Walport MH, et al. The Complement System and Innate Immunity. Immunobiology: The Immune System in Health and Disease. 5th ed. New York, NY: Garland Science; 2001.
58. Walport MJ. Complement. First of two parts. N Engl J Med 2001;344:1058–1066.
59. Walport MJ. Complement. Second of two parts. N Engl J Med 2001;344:1140–1144.
60. Lachmann PJ. The amplification loop of the complement pathways. Adv Immunol 2009;104:115–149.
61. Zipfel PF, Skerka C. Complement regulators and inhibitory proteins. Nat Rev Immunol 2009;9:729–740.
62. Ricklin D, Hajishengallis G, Yang K, Lambris JD. Complement: a key system for immune surveillance and homeostasis. Nat Immunol 2010;11:785–797.
63. Fritsche LG, Fariss RN, Stambolian D, et al. Age-related macular degeneration: genetics and biology coming together. Annu Rev Genomics Hum Genet 2014;15:151–171.
64. Schramm EC, Clark SJ, Triebwasser MP, et al. Genetic variants in the complement system predisposing to age-related macular degeneration: a review. Mol Immunol 2014;61:118–125.
65. Volanakis JE, Narayana SV. Complement factor D, a novel serine protease. Protein Sci 1996;5:553–564.
66. Lesavre PH, Muller-Eberhard HJ. Mechanism of action of factor D of the alternative complement pathway. J Exp Med 1978;148:1498–1509.
67. Law SK, Dodds AW. The internal thioester and the covalent binding properties of the complement proteins C3 and C4. Protein Sci 1997;6:263–274.
68. Harboe M, Garred P, Karlstrom E, et al. The down-stream effects of mannan-induced lectin complement pathway activation depend quantitatively on alternative pathway amplification. Mol Immunol 2009;47:373–380.
69. Harboe M, Ulvund G, Vien L, et al. The quantitative role of alternative pathway amplification in classical pathway induced terminal complement activation. Clin Exp Immunol 2004;138:439–446.
70. Lachmann PJ, Halbwachs L. The influence of C3b inactivator (KAF) concentration on the ability of serum to support complement activation. Clin Exp Immunol 1975;21:109–114.
71. Cole DS, Hughes TR, Gasque P, Morgan BP. Complement regulator loss on apoptotic neuronal cells causes increased complement activation and promotes both phagocytosis and cell lysis. Mol Immunol 2006;43:1953–1964.
72. Stevens B, Allen NJ, Vazquez LE, et al. The classical complement cascade mediates CNS synapse elimination. Cell 2007;131:1164–1178.
73. Stephan AH, Barres BA, Stevens B. The complement system: an unexpected role in synaptic pruning during development and disease. Annu Rev Neurosci 2012;35:369–389.
74. Barbu A, Hamad OA, Lind L, et al. The role of complement factor C3 in lipid metabolism. Mol Immunol 2015;67:101–107.
75. Schoengraf P, Lambris JD, Recknagel S, et al. Does complement play a role in bone development and regeneration? Immunobiology 2013;218:1–9.
76. Hollyfield JG, Bonilha VL, Rayborn ME, et al. Oxidative damage-induced inflammation initiates age-related macular degeneration. Nat Med 2008;14:194–198.
77. Klein RJ, Zeiss C, Chew EY, et al. Complement factor H polymorphism in age-related macular degeneration. Science 2005;308:385–389.
78. Edwards AO, Ritter R III, Abel KJ, et al. Complement factor H polymorphism and age-related macular degeneration. Science 2005;308:421–424.
79. Haines JL, Hauser MA, Schmidt S, et al. Complement factor H variant increases the risk of age-related macular degeneration. Science 2005;308:419–421.
80. Hageman GS, Anderson DH, Johnson LV, et al. A common haplotype in the complement regulatory gene factor H (HF1/CFH) predisposes individuals to age-related macular degeneration. Proc Natl Acad Sci U S A 2005;102:7227–7232.
81. Fritsche LG, Chen W, Schu M, et al. Seven new loci associated with age-related macular degeneration. Nat Genet 2013;45:433–439. 439e431-432.
82. Helgason H, Sulem P, Duvvari MR, et al. A rare nonsynonymous sequence variant in C3 is associated with high risk of age-related macular degeneration. Nat Genet 2013;45:1371–1374.
83. Raychaudhuri S, Iartchouk O, Chin K, et al. A rare penetrant mutation in CFH confers high risk of age-related macular degeneration. Nat Genet 2011;43:1232–1236.
84. Seddon JM, Yu Y, Miller EC, et al. Rare variants in CFI, C3 and C9 are associated with high risk of advanced age-related macular degeneration. Nat Genet 2013;45:1366–1370.
85. van de Ven JP, Nilsson SC, Tan PL, et al. A functional variant in the CFI gene confers a high risk of age-related macular degeneration. Nat Genet 2013;45:813–817.
86. Yu Y, Triebwasser MP, Wong EK, et al. Whole-exome sequencing identifies rare, functional CFH variants in families with macular degeneration. Hum Mol Genet 2014;23:5283–5293.
87. Zhan X, Larson DE, Wang C, et al. Identification of a rare coding variant in complement 3 associated with age-related macular degeneration. Nat Genet 2013;45:1375–1379.
88. Manuelian T, Hellwage J, Meri S, et al. Mutations in factor H reduce binding affinity to C3b and heparin and surface attachment to endothelial cells in hemolytic uremic syndrome. J Clin Invest 2003;111:1181–1190.
89. Prosser BE, Johnson S, Roversi P, et al. Structural basis for complement factor H linked age-related macular degeneration. J Exp Med 2007;204:2277–2283.
90. Atkinson JP, Goodship TH. Complement factor H and the hemolytic uremic syndrome. J Exp Med 2007;204:1245–1248.
91. Wright AF. A rare variant in CFH directly links age-related macular degeneration with rare glomerular nephropathies. Nat Genet 2011;43:1176–1177.
92. Kavanagh D, Yu Y, Schramm EC, et al. Rare genetic variants in the CFI gene are associated with advanced age-related macular degeneration and commonly result in reduced serum factor I levels. Hum Mol Genet 2015;24:3861–3870.
93. Scholl HP, Charbel Issa P, Walier M, et al. Systemic complement activation in age-related macular degeneration. PLoS One 2008;3:e2593.
94. Reynolds R, Hartnett ME, Atkinson JP, et al. Plasma complement components and activation fragments: associations with age-related macular degeneration genotypes and phenotypes. Invest Ophthalmol Vis Sci 2009;50:5818–5827.
95. Stanton CM, Yates JR, den Hollander AI, et al. Complement factor D in age-related macular degeneration. Invest Ophthalmol Vis Sci 2011;52:8828–8834.
96. Silva AS, Teixeira AG, Bavia L, et al. Plasma levels of complement proteins from the alternative pathway in patients with age-related macular degeneration are independent of complement factor H Tyr(4)(0)(2)His polymorphism. Mol Vis 2012;18:2288–2299.
97. Loyet KM, Deforge LE, Katschke KJ Jr., et al. Activation of the alternative complement pathway in vitreous is controlled by genetics in age-related macular degeneration. Invest Ophthalmol Vis Sci 2012;53:6628–6637.
98. Johnson LV, Leitner WP, Staples MK, Anderson DH. Complement activation and inflammatory processes in Drusen formation and age related macular degeneration. Exp Eye Res 2001;73:887–896.
99. Johnson LV, Ozaki S, Staples MK, et al. A potential role for immune complex pathogenesis in drusen formation. Exp Eye Res 2000;70:441–449.
100. Mullins RF, Russell SR, Anderson DH, Hageman GS. Drusen associated with aging and age-related macular degeneration contain proteins common to extracellular deposits associated with atherosclerosis, elastosis, amyloidosis, and dense deposit disease. FASEB J 2000;14:835–846.
101. Johnson PT, Betts KE, Radeke MJ, et al. Individuals homozygous for the age-related macular degeneration risk-conferring variant of complement factor H have elevated levels of CRP in the choroid. Proc Natl Acad Sci U S A 2006;103:17456–17461.
102. Newman AM, Gallo NB, Hancox LS, et al. Systems-level analysis of age-related macular degeneration reveals global biomarkers and phenotype-specific functional networks. Genome Med 2012;4:16.
103. Mullins RF, Dewald AD, Streb LM, et al. Elevated membrane attack complex in human choroid with high risk complement factor H genotypes. Exp Eye Res 2011;93:565–567.
104. Whitmore SS, Sohn EH, Chirco KR, et al. Complement activation and choriocapillaris loss in early AMD: implications for pathophysiology and therapy. Prog Retin Eye Res 2015;45:1–29.
105. Vogt SD, Curcio CA, Wang L, et al. Retinal pigment epithelial expression of complement regulator CD46 is altered early in the course of geographic atrophy. Exp Eye Res 2011;93:413–423.
106. Ebrahimi KB, Fijalkowski N, Cano M, Handa JT. Decreased membrane complement regulators in the retinal pigmented epithelium contributes to age-related macular degeneration. J Pathol 2013;229:729–742.
107. Seddon JM, Gensler G, Rosner B. C-reactive protein and CFH, ARMS2/HTRA1 gene variants are independently associated with risk of macular degeneration. Ophthalmology 2010;117:1560–1566.
108. Robman L, Baird PN, Dimitrov PN, et al. C-reactive protein levels and complement factor H polymorphism interaction in age-related macular degeneration and its progression. Ophthalmology 2010;117:1982–1988.
109. Cao S, Ko A, Partanen M, et al. Relationship between systemic cytokines and complement factor H Y402H polymorphism in patients with dry age-related macular degeneration. Am J Ophthalmol 2013;156:1176–1183.
110. Shaw PX, Zhang L, Zhang M, et al. Complement factor H genotypes impact risk of age-related macular degeneration by interaction with oxidized phospholipids. Proc Natl Acad Sci U S A 2012;109:13757–13762.
111. Smailhodzic D, Klaver CC, Klevering BJ, et al. Risk alleles in CFH and ARMS2 are independently associated with systemic complement activation in age-related macular degeneration. Ophthalmology 2012;119:339–346.
112. Ding JD, Kelly U, Groelle M, et al. The role of complement dysregulation in AMD mouse models. Adv Exp Med Biol 2014;801:213–219.
113. Coffey PJ, Gias C, McDermott CJ, et al. Complement factor H deficiency in aged mice causes retinal abnormalities and visual dysfunction. Proc Natl Acad Sci U S A 2007;104:16651–16656.
114. Ding JD, Kelly U, Landowski M, et al. Expression of human complement factor H prevents age-related macular degeneration-like retina damage and kidney abnormalities in aged cfh knockout mice. Am J Pathol 2015;185:29–42.
115. Ufret-Vincenty RL, Aredo B, Liu X, et al. Transgenic mice expressing variants of complement factor H develop AMD-like retinal findings. Invest Ophthalmol Vis Sci 2010;51:5878–5887.
116. Cashman SM, Desai A, Ramo K, Kumar-Singh R. Expression of complement component 3 (C3) from an adenovirus leads to pathology in the murine retina. Invest Ophthalmol Vis Sci 2011;52:3436–3445.
117. Rohrer B, Guo Y, Kunchithapautham K, Gilkeson GS. Eliminating complement factor D reduces photoreceptor susceptibility to light-induced damage. Invest Ophthalmol Vis Sci 2007;48:5282–5289.
118. Sweigard JH, Matsumoto H, Smith KE, et al. Inhibition of the alternative complement pathway preserves photoreceptors after retinal injury. Sci Transl Med 2015;7:297ra116.
119. Zhou J, Jang YP, Kim SR, Sparrow JR. Complement activation by photooxidation products of A2E, a lipofuscin constituent of the retinal pigment epithelium. Proc Natl Acad Sci U S A 2006;103:16182–16187.
120. Zhou J, Kim SR, Westlund BS, Sparrow JR. Complement activation by bisretinoid constituents of RPE lipofuscin. Invest Ophthalmol Vis Sci 2009;50:1392–1399.
121. Woodell A, Coughlin B, Kunchithapautham K, et al. Alternative complement pathway deficiency ameliorates chronic smoke-induced functional and morphological ocular injury. PLoS One 2013;8:e67894.
122. Broz P, Dixit VM. Inflammasomes: mechanism of assembly, regulation and signalling. Nat Rev Immunol 2016;16:407–420.
123. Tarallo V, Hirano Y, Gelfand BD, et al. DICER1 loss and Alu RNA induce age-related macular degeneration via the NLRP3 inflammasome and MyD88. Cell 2012;149:847–859.
124. Kim Y, Tarallo V, Kerur N, et al. DICER1/Alu RNA dysmetabolism induces Caspase-8-mediated cell death in age-related macular degeneration. Proc Natl Acad Sci U S A 2014;111:16082–16087.
125. Doyle SL, Campbell M, Ozaki E, et al. NLRP3 has a protective role in age-related macular degeneration through the induction of IL-18 by drusen components. Nat Med 2012;18:791–798.
126. Kaneko H, Dridi S, Tarallo V, et al. DICER1 deficit induces Alu RNA toxicity in age-related macular degeneration. Nature 2011;471:325–330.
127. Anderson OA, Finkelstein A, Shima DT. A2E induces IL-1ss production in retinal pigment epithelial cells via the NLRP3 inflammasome. PLoS One 2013;8:e67263.
128. Liu RT, Gao J, Cao S, et al. Inflammatory mediators induced by amyloid-beta in the retina and RPE in vivo: implications for inflammasome activation in age-related macular degeneration. Invest Ophthalmol Vis Sci 2013;54:2225–2237.
129. Asgari E, Le Friec G, Yamamoto H, et al. C3a modulates IL-1beta secretion in human monocytes by regulating ATP efflux and subsequent NLRP3 inflammasome activation. Blood 2013;122:3473–3481.
130. Samstad EO, Niyonzima N, Nymo S, et al. Cholesterol crystals induce complement-dependent inflammasome activation and cytokine release. J Immunol 2014;192:2837–2845.
131. Laudisi F, Spreafico R, Evrard M, et al. Cutting edge: the NLRP3 inflammasome links complement-mediated inflammation and IL-1beta release. J Immunol 2013;191:1006–1010.
132. Triantafilou K, Hughes TR, Triantafilou M, Morgan BP. The complement membrane attack complex triggers intracellular Ca2+ fluxes leading to NLRP3 inflammasome activation. J Cell Sci 2013;126:2903–2913.
133. Doyle SL, Adamson P, Lopez FJ, et al. Reply to IL-18 is not therapeutic for neovascular age-related macular degeneration. Nat Med 2014;20:1376–1377.
134. Hirano Y, Yasuma T, Mizutani T, et al. IL-18 is not therapeutic for neovascular age-related macular degeneration. Nat Med 2014;20:1372–1375.
135. Doyle SL, Ozaki E, Brennan K, et al. IL-18 attenuates experimental choroidal neovascularization as a potential therapy for wet age-related macular degeneration. Sci Transl Med 2014; 6:230ra44.
136. Age-Related Eye Disease Study Research Group. Risk factors associated with age-related macular degeneration. A case-control study in the age-related eye disease study: Age-Related Eye Disease Study report number 3. Ophthalmology 2000;107:2224–2232.
137. Clemons TE, Milton RC, Klein R, et al. Risk factors for the incidence of advanced age-related macular degeneration in the Age-Related Eye Disease Study (AREDS) AREDS report no. 19. Ophthalmology 2005;112:533–539.
138. Schmitz-Valckenberg S, Sahel JA, Danis R, et al. Natural history of geographic atrophy progression secondary to age-related macular degeneration (Geographic Atrophy Progression Study). Ophthalmology 2016;123:361–368.
139. Leung E, Landa G. Update on current and future novel therapies for dry age-related macular degeneration. Expert Rev Clin Pharmacol 2013;6:565–579.
140. Kvanta A, Grudzinska MK. Stem cell-based treatment in geographic atrophy: promises and pitfalls. Acta Ophthalmol 2014;92:21–26.
141. Fowler BJ, Gelfand BD, Kim Y, et al. Nucleoside reverse transcriptase inhibitors possess intrinsic anti-inflammatory activity. Science 2014;346:1000–1003.
142. Boyd SR, Zhao X, Joshi R, et al. Modulation of innate immunity protects against induction and expansion of Geographic Atrophy (GA) in a rodent model of dry age related macular degeneration (AMD). ARVO Meet Abstr 2014;55:1241.
143. Apellis Pharmaceuticals to acquire Potentia Pharmaceuticals. 2014. Available at: http://http://www.potentiapharma.com/about/news.htm#30. Accessed July 17, 2015.
144. Soliris (eculizumab) Prescribing Information. 2014. Available at: http://soliris.net/resources/pdf/soliris_pi.pdf. Accessed November 24, 2015.
145. Alexion research & development: pipeline. Available at: http://alxn.com/research-development/pipeline. Accessed February 27, 2015.
146. Ralston P, Sloan D, Waters-Honcu D. A pilot, open-label study of the safety of MC-1101 in both normal volunteers and patients with early nonexudative age-related macular degeneration. ARVO Meet Abstr 2010;51:913.
147. Katschke KJ Jr., Wu P, Ganesan R, et al. Inhibiting alternative pathway complement activation by targeting the factor D exosite. J Biol Chem 2012;287:12886–12892.
148. Loyet KM, Good J, Davancaze T, et al. Complement inhibition in cynomolgus monkeys by anti-factor D antigen-binding fragment for the treatment of an advanced form of dry age-related macular degeneration. J Pharmacol Exp Ther 2014;351:527–537.
149. Le KN, Gibiansky L, Good J, et al. A mechanistic pharmacokinetic/pharmacodynamic model of factor D inhibition in cynomolgus monkeys by lampalizumab for the treatment of geographic atrophy. J Pharmacol Exp Ther 2015;355:288–296.
150. Do DV, Pieramici DJ, van Lookeren Campagne M, et al. A phase IA dose-escalation study of the anti-factor D monoclonal antibody fragment FCFD4514S in patients with geographic atrophy. Retina 2014;34:313–320.
151. Le KN, Gibiansky L, van Lookeren Campagne M, et al. Population pharmacokinetics and pharmacodynamics of lampalizumab administered intravitreally to patients with geographic atrophy. CPT Pharmacometrics Syst Pharmacol 2015;4:595–604.
Keywords:

age-related macular degeneration; atrophy; complement; eculizumab; geographic atrophy; lampalizumab

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