Open Access
Review
Issue
Parasite
Volume 22, 2015
Article Number 10
Number of page(s) 20
DOI https://doi.org/10.1051/parasite/2015010
Published online 18 February 2015

© J. Lorenzo-Morales et al., published by EDP Sciences, 2015

Licence Creative Commons
This is an Open Access article distributed under the terms of the Creative Commons Attribution License (http://creativecommons.org/licenses/by/4.0), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

1. Introduction – What is Acanthamoeba keratitis?

Acanthamoeba species are the causative agents of a sight-threatening infection of the cornea known as Acanthamoeba keratitis (AK) (Fig. 1). Interestingly, AK is increasingly being recognized as a severe sight-threatening ocular infection, worldwide. Although contact lens (CL) wear is the leading risk factor for AK, Acanthamoeba spp. can cause infection in non-contact lens wearers. Patients with AK may experience pain with photophobia, ring-like stromal infiltrate, epithelial defect and lid oedema. If AK is not treated adequately and aggressively, it can lead to loss of vision [18, 46, 47, 56, 87, 111, 112, 117].

thumbnail Figure 1.

(A) Corneal melting and vascularization in a patient with Acanthamoeba keratitis. (B) Observed corneal damage in AK is shown after sodium fluorescein application. Original.

Diagnosis of AK is challenging, and the available treatments are lengthy and not fully effective against all strains. Moreover, the pathogenesis of Acanthamoeba keratitis is still under study, and the identification of the key factors involved in this process should be useful for the development of fully effective therapies. The current difficulty in effective treatment is due to the resistant cyst stage of Acanthamoeba. Together with common misdiagnosis of AK in most cases and a lack of a consensus for AK diagnosis, AK has remained significant. Nevertheless, AK is still considered a rare disease and is included in the Orphanet database (ORPHA67043) and with an estimated prevalence of 1–9/100,000.

2. Diagnostics of AK

The most important step in AK diagnosis is to think of it. Generally, AK should be considered in all contact lens wearers and in any case of corneal trauma with exposure to soil or contaminated water [20, 23, 36, 54]. Common symptoms are massive pain, photophobia and tearing. The sooner the disease is diagnosed, the better the outcome [6, 12, 54, 99, 104]. If diagnosis is delayed, the amoebae have already penetrated deeply into the corneal stroma and successful therapy becomes exceedingly difficult. AK is usually unilateral and progresses slowly, from epithelial to stromal disease. At the beginning of the infection, a diffuse superficial keratopathy is found, later multifocal infiltrates are almost always observed in the stroma. Acanthamoeba sclerokeratitis is an uncommon complication of AK and assumedly has an immune-mediated origin. Tu et al. [104] established five levels of AK severity based on slit-lamp biomicroscopy findings: epitheliitis, epitheliitis with radial neuritis, anterior stromal disease, deep stromal keratitis, or ring infiltrate. The characteristic ring infiltrate is, however, only seen in approximately 50% of patients. In the early stage, AK can easily be confused with Herpes simplex keratitis, while in the advanced stage, the infection resembles the clinical picture of a fungal keratitis or a corneal ulcer (Table 1).

Table 1.

Important characteristics for the differential diagnosis of Acanthamoeba keratitis (AK) compared to keratitis due to other infectious agents.

Contact lens wearers typically seek medical help late, because they are used to minor irritations in the eye.

The tentative diagnosis of AK can often be made by in vivo confocal microscopy (IVCM). The Acanthamoeba cysts appearing as hyper-reflective, spherical structures are usually well defined because of their double wall; the trophozoites are difficult to distinguish from leukocytes and keratocyte nuclei [110]. However, the direct detection of the causative agent in a corneal scrape specimen is the only reliable diagnostic method for AK. Culture remains the gold standard of Acanthamoeba laboratory diagnosis, but today several PCR-based techniques are also well established and usually increase sensitivity significantly [41, 59, 84, 90]. In cases of severe infection, amoeba density is sometimes very high and the amoebae can already be detected by direct microscopy of the clinical sample, without enrichment. Acanthamoeba trophozoites or cysts are readily recognizable in phase contrast microscopy, but also stain well in several stains and cysts exhibit auto-fluorescence [46, 54]. However, particularly if patients have already been pre-treated with antibiotics, amoeba density is usually very low. Moreover, amoebae exhibit altered morphologies – in these cases, even culture often remains negative and molecular techniques are indispensable. Reliable identification below the genus level requires genotyping. Serological techniques are of no diagnostic value as specific antibodies are also detected in apparently healthy people due to the ubiquity of Acanthamoeba.

In contrast to infections with other amoebae, acanthamoebae can form cysts within the tissue. As a single cyst surviving in the cornea can lead to reinfection, the progress of therapy should be checked regularly. An ongoing infection should be monitored every 1–2 weeks. After clinical recovery, monthly checks are sufficient, ideally until 6 months after decline of symptoms.

In most countries, the vast majority of AK cases occur in CL wearers and AK can be prevented extensively by strict contact lens hygiene. Typically, singular amoebae gain access to the lens case via tap water or the air, rapidly grow to high densities within the lens case if this is not cleaned properly and regularly, and then attach to the lenses and infect the eye [116]. Wearers of soft contact lenses using multipurpose solutions are at particular risk, because acanthamoebae adhere especially well to the hydrophilic plastic of these lenses, and soft lenses are more difficult to clean than rigid lenses. Moreover, soft lenses are often over worn (dailies used for several days, monthlies used for several months) and are also the type of lenses used by people who do not regularly but only occasionally (e.g. once a week for sports) wear their contacts, and who are often unaware of proper contact lens hygiene. For prophylaxis of AK, lens cases should be cleaned manually and air dried, contact lenses should be cleaned and stored using an appropriate (best: two-step) contact lens cleaning system, and both, lenses and lens cases have to be exchanged regularly.

2.1. Material

For confirmation of an AK, sampling and investigation of the correct material is crucial. Only if amoebae are detected in corneal scrapings or in corneal biopsies a reliable diagnosis can be made. Acanthamoebae penetrate the cornea and are usually not found on the corneal surface, thus superficial swab samples or tear samples often remain negative, particularly in the advanced stage of the disease and/or if patients have already been pretreated with antibiotics. On the contrary, contact lens containers, even those of entirely healthy CL wearers, are almost always positive for acanthamoebae, at least in PCR. This means that the detection of Acanthamoeba spp. in the CL case does not necessarily indicate an AK. When the CL case is negative, however, it is very unlikely that the patient has an AK, unless, of course, the CL case was recently changed.

The optimal material for AK diagnosis is a corneal scraping/biopsy stored in 200 μL of sterile saline (amoeba saline* or PBS or 0.9% NaCl) in order to prevent desiccation.

*See Table 2.

Table 2.

Neff’s Amoeba Saline (AS) [71]. 10 mL of each stock solution (10×) are added to 950 mL dH2O, mixed, sterilized by filtration and aliquoted into needed volumes.

2.2. Sample preparation

A major challenge in AK diagnostics is the many different types of sample material on the one hand, and sample transport media and containers on the other. Below, we have attempted to provide a guideline for sample preparation depending on the type of material received. A general overview of the diagnostic procedure is given in Figure 2.

thumbnail Figure 2.

Overview of the diagnostic procedure for Acanthamoeba keratitis.

When a corneal scraping/biopsy is received, the sample itself is used for DNA isolation, while the transport medium (ideally 200 μL of sterile saline) is used for culture. Larger tissue samples can be cut into two halves, of which one can be transferred onto an agar plate and the other used for DNA isolation. When the sample is received in >200 μL of transport medium, the sample is used for DNA isolation and the transport medium is shaken well, centrifuged at 700 g/7 min, resuspended in 200 μL of sterile saline and processed as described above.

When only liquid is received (e.g. contact lens solution), samples ≤200 μL should be mixed and split into two aliquots directly upon receipt, one aliquot is then used for culture, the other aliquot is used for DNA isolation. Liquid samples >200 μL are centrifuged at 700 g/7 min, resuspended in 200 μL of sterile saline and processed as described above.

Contact lenses or swabs are shaken vigorously in the original transport medium (contact lens solution/sterile saline) and the lens/swab is then inoculated onto an agar plate and the liquid can be used for DNA isolation. When contact lens cases are received, the liquid is processed as described above, but a biofilm swab from the inner surface should also be taken and inoculated onto a plate culture.

When fixed material is received (swabs/contact lens case cell pellets/tissue samples fixed either in ethanol or formalin or embedded in paraffin or as stained sections on microscopic slides), it is recommended to perform staining (lactophenol cotton blue and/or immunostaining) and/or PCR. However, it is important to isolate the DNA using a suitable protocol for the respective material and to adapt the PCR protocol for fragmented DNA, particularly when the material is formalin-fixed (i.e. amplicons should not exceed 300 bp in length).

2.3. Direct microscopy

In severe infections or when highly contaminated contact lens cases are investigated, the amoebae can usually already be detected by direct microscopy (200×–400× magnification) of the original sample. For microscopic investigation of amoebae, phase contrast or interference contrast are particularly well suited. Nucleated corneal cells of lower cornea layers may resemble amoebae, but acanthamoebae can be discriminated from other mononuclear cells by their large central nucleolus, their contractile vacuole and their hyaline pseudopodia with characteristic hyaline protrusions, the so-called acanthopodia. The trophozoites are 15–45 μm in size and have an oval to elongated outline (Fig. 3). They move slowly by forming usually one or two pseudopodia in the direction of movement. The cysts are smaller (12–25 μm) and polygonal or star-shaped (Fig. 4). They have two cyst walls which are connected at several points. These points of contact between endocyst and ectocyst are covered by an operculum, which is removed during excystation.

thumbnail Figure 3.

Acanthamoeba trophozoites with the characteristic acanthopodia (A) in phase contrast, (B) in bright field microscopy. Scale bar: 10 μm. Originals.

thumbnail Figure 4.

Acanthamoeba cysts in interference contrast microscopy (A) morphological group I, (B) morphological group II, (C) morphological group III. Scale bar: 10 μm. Original.

2.4. Stains

Stains are practical for the detection of cysts in fresh clinical material or in pelleted lens-case solution and for the investigation of tissue sections. Fast and easy stains are lactophenol-cotton blue or Giemsa, but also calcofluor white and acridine orange usually give very good results. If morphological details are to be studied, it is recommended to use a silver stain, which is particularly well-suited for the investigation of the cysts. However, amoebae have to be cultured prior to staining. A general problem is that other cells, particularly fungi also stain well in these stains. As a specific staining, immunostaining using anti-Acanthamoeba antibodies is recommended which is also the stain of choice for tissue sections. Alternatively, tissue section can be stained with haematoxylin & eosin (HE) [35].

2.4.1. Lactophenol-cotton blue (LPCB)

The material is mixed with an adequate volume of LPCB stain (20 g phenol crystals, 20 mL lactic acid, 40 mL glycerol, 0.05 g cotton-blue and 20 mL dH2O; or ready-mixed available through e.g. Sigma-Aldrich) and investigated by light microscopy [101]. This stain is particularly well suited for Acanthamoeba cysts; the cyst walls and the nucleus appear in an intensive blue, while the cytoplasm stains light-blue.

2.4.2. Acridine orange

Samples are fixed in 95% methanol for 2 min onto a glass slide, air dried, covered with acridine orange staining solution (pH 4) for 2 min, rinsed with H2O and air dried. Cysts appear bright orange and are easily discernible in fluorescence microscopy.

2.4.3. Calcofluor white

Samples are transferred to a glass slide, air dried and fixed for 3 min with methanol. Subsequently, the sample is rinsed in PBS and stained using 2–3 drops of calcofluor white solution (0.1%, e.g. Sigma-Aldrich or Thermo Scientific). After 5 min, the slide is rinsed with PBS and counter-stained with Evan’s blue (0.05%, e.g. Sigma-Aldrich or Thermo Scientific) for several seconds. It is important to use an embedding solution without auto-fluorescence. Slides are investigated by fluorescence microscopy (300–440 nm). Acanthamoeba cysts appear in a light green because the calcofluor white binds to the cellulose in the cyst walls. Evan’s blue diminishes the background fluorescence making the trophozoites appear reddish-brown.

2.4.4. Silver

The cysts are harvested from a culture plate/flask, suspended in 2 mL amoeba saline (Table 2) and washed three times in amoeba saline by centrifugation (500 g/10 min). The sample is fixed for 20 min in 2% formalin and washed in amoeba saline, the supernatant is removed and the pellet is transferred to a glass slide using an inoculating loop and mixed with Mayer’s albumin (glycerine-albumin 1:1, e.g. Hardy Diagnostics). Then, the cysts are fixed onto the slide using Clarke’s fixative (95% alcohol-acetic acid 9:1) for 2 h. The fixative is removed using dH2O and the slides are incubated in 0.5% silver-protein solution in a water bath at 60 °C. After 2 h, the slides are transferred to the reducing agent (1% hydroquinone in 5% Na2SO3) and incubated during gentle shaking for several seconds up to 5 min. The slides are washed in dH2O, dehydrated in an alcohol series, cleared with xylene, mounted and investigated by bright field microscopy.

2.4.5. Immunostain

To the best of our knowledge, no commercial kit is available, but antisera against the three Acanthamoeba groups (I–III), produced by immunization of a rabbit with Acanthamoeba whole-cell antigen, are available in many laboratories (including our own) and can be obtained upon request.

2.4.6. Haematoxylin & eosin (HE)

The tissue section is fixed in 10% neutral buffered formalin solution (e.g. Sigma-Aldrich). Serial sections of 6 μm are produced, deparaffinized for 1–2 min in xylene, dehydrated in alcohol and washed with dH2O. Subsequently, the sample is stained with haematoxylin and eosin, washed, covered with a cover slip and investigated by bright field microscopy.

2.5. Culture

The gold standard for Acanthamoeba detection is still the plate culture technique [71, 91]. The material (corneal scrapings/biopsies or transport medium/contact lenses/swabs, etc.) is applied centrally onto a 90 mm 1.5% non-nutrient (NN) agar plate covered with a lawn (100 μL) of a 24 h old culture of non-mucous bacteria (e.g. Escherichia coli). Plates are sealed with Parafilm®, incubated at 30 °C and screened daily for amoebae, optimally by inverted phase contrast microscopy. In cases of severe infection, amoebae are usually already visible after 24–48 h (Fig. 5). However, samples should be observed for up to 1 week to reliably prove a negative result. Alternatively, amoebae can be cultured in tissue culture flasks in a suspension of bacteria in PBS.

thumbnail Figure 5.

Acanthamoeba trophozoites observed in culture in a case of severe AK infection.

In culture, acanthamoebae form cysts within approximately 1 week (depending on temperature and availability of nutrients). These cysts can be identified at least down to the morphological group level (Acanthamoeba sp. group I–III) based on size, morphology and number of opercula [80] (Fig. 4). Most AK cases are caused by representatives of group II (Fig. 4B), but group III strains have also been described as causative agents of AK. Group II strains have polygonal cysts with 3–7 cyst arms, while group III strains are rounded and do not have clearly visible cyst arms. Group I strains with their large and beautifully star-shaped cysts have not (yet?) been described to cause AK. Species identification can be achieved using the identification key by Page [71]. However, in some cases, morphological identification is ambiguous and the validity of some described species has been questioned altogether.

If the isolated amoebae are needed for further studies (e.g. genotyping), sub-cultures should be prepared since fungi and other microorganisms also grow very well in these cultures. In addition, several physiological properties can be used to further describe and discriminate Acanthamoeba isolates, including growth rate, temperature tolerance, cell culture pathogenicity and in vivo mouse pathogenicity [22, 24, 34, 115].

2.5.1. Sub-culture

From positive samples, clonal cultures can be prepared by transferring a small piece (<1 cm2) of agar with only few clean cysts on it (optimally a single cyst using a micromanipulator) upside down to a fresh plate. Plates should be sub-cultured every 2–4 weeks.

Monoxenic plates sealed with Parafilm® can be kept for several months at room temperature. If they do not entirely dehydrate, cysts remain viable for many years.

2.5.1.2. Temperature tolerance

Sub-cultures can be used for investigating the temperature tolerance of the respective isolate. Parallel cultures are incubated at 30 °C, 37 °C and 42 °C, respectively. The temperature of the human eye is approximately 34 °C. Usually however, the ability to grow at 37 °C (body temperature) and 42 °C (high fever) is also investigated. Plates are investigated daily by phase contrast microscopy.

2.5.2. Axenisation

Acanthamoebae can be axenised by harvesting cysts from the plate cultures and incubating them in 3% HCl overnight in order to eliminate the bacteria. It is usually sufficient to install three parallel plate cultures and wait for cyst formation (usually approximately 2 weeks). It is important that cysts be fully mature, because otherwise they will not survive the acid treatment. Subsequently, the cysts are washed 2–3× in amoeba saline (700 g/7 min) to remove remaining acid and transferred to liquid cultures. An easy culture medium for acanthamoebae is proteose peptone-yeast extract-glucose (PYG) [71] (Table 3).

Table 3.

PYG medium [71]. Compounds are weighted into a 1 L bottle, filled up to 1 L with dH2O, mixed and sterilized by filtration.

To keep axenic cultures running, medium has to be changed ideally every 1–2 weeks. The cultures should be checked regularly for bacterial contamination (e.g. by transferring an aliquot of the supernatant to bacterial broth), as should the amoebae themselves for endocytobionts. To reduce the risk of contamination, antibiotics (e.g. 200 IU penicillin and 200 μg/mL streptomycin) and/or antimycotics (e.g. amphotericin B) can be added to the culture medium.

Liquid culture is not suited to initial clinical samples, as bacteria and fungi would overgrow the cultures (a clinical sample from the eye surface is never sterile).

2.5.3. Cell culture pathogenicity

Trophozoites are harvested from axenic cultures by centrifugation (700 g/7 min.) and transferred onto a monolayer of human (e.g. HeLA, HEp-2 or keratinocytes) or animal cells (e.g. VERO) in an amoeba/cell ratio of 1:10. The amoebae are designated as highly cytopathic, when the monolayer is completely lysed within 24 h.

2.5.4. Mouse inoculation

Trophozoites are harvested from axenic cultures by centrifugation (700 g/7 min.), re-suspended in sterile PBS and inoculated into mice intra-nasally or intra-cerebrally. Young mice are generally more susceptible to an Acanthamoeba infection. Pathogenic strains lead to death within a few days up to 4 weeks. Importantly, amoebae can lose their pathogenicity during long-term axenic laboratory culture.

2.6. DNA isolation

For genotyping, actively growing amoebae (~106 cells) are harvested from culture plates and resuspended in 100 μL of sterile 0.9% NaCl for DNA isolation. Whole-cell DNA can be isolated from the amoebal suspensions using a commercial DNA isolation kit following the manufacturer’s protocol for the respective type of material. When larger tissue samples are received, we recommend homogenization of the material prior to DNA isolation.

2.7. PCR/real-time PCR

The most frequently used PCR for Acanthamoeba diagnostics is probably the one established by Schroeder et al. [90, 97] amplifying a fragment of the 18S rRNA gene using the JDP1 (5′-GGCCCAGATCGTTTACCGTGAA-3′) and JDP2 (5′-TCTCACAAGCTGCTAGGGAGTCA-3′) primers. In this PCR, the length of the amplicon varies between 423 and 551 bp depending on the genotype, and DNA sequencing of the amplicon allows for genotyping in most cases. Generally, whichever diagnostic PCR is used, it should be run with at least two different dilutions from each sample (as the proportion amoebal DNA: human DNA can vary greatly) and a genotype T4 reference strain should be used as a positive and DNA-free water as a negative control. Amplicons are visualized by agarose-gel electrophoresis and, if genotyping is required, the respective bands are extracted from the gel, purified and subjected to DNA sequencing.

For samples that had been fixed in formaldehyde, we employ a modified PCR using the JDP1 primer from the PCR described above and the P2r primer (5′-GACTACGACGGTATCTGATC-3′) [113], which amplifies a shorter (~300 bp) fragment of the 18S rRNA gene.

In the past years, several protocols for real-time PCR have also been published [43, 61, 81, 84]. A highly sensitive and specific assay is the multiplex real-time PCR established by Qvarnstrom et al. [81], which for AK diagnostics can also be run as a singleplex.

2.8. Genotyping

Sequences of the PCR amplicons can be obtained by direct sequencing or by cloning. Generally, it is recommended to obtain sequences from both strands and assemble them to give a consensus sequence. For genotyping, obtained sequences are compared to sequences of Acanthamoeba reference strains by multiple alignments with all available genotypes at that time (currently 19) with the model assumption of a <5% sequence dissimilarity within one genotype as established by Gast et al. [33] and Stothard et al. [97]. Worldwide, the vast majority of AK cases are caused by Acanthamoeba genotype T4, but genotypes T3 and T11 are also commonly associated with AK, and in fact most genotypes known to date have at least once been involved in an AK case [11, 116].

3. Pathogenesis of Acanthamoeba keratitis

The devastating nature of Acanthamoeba keratitis and the problems associated with its diagnosis and successful therapy suggest a need for complete understanding of the pathogenesis and pathophysiology to find alternative therapeutic interventions. Another major concern during the course of therapy is the ability of Acanthamoeba to transform into dormant cyst forms, which may resist recommended levels of antimicrobial chemotherapy. The ability of Acanthamoeba to produce infection requires specific adhesins, production of toxins, and its ability to resist immune/environmental factors and chemotherapeutic agents, which likely enable this pathogen to produce infection. For simplicity, the information is divided into factors contributing directly and indirectly to Acanthamoeba pathogenicity (Fig. 6).

thumbnail Figure 6.

Factors contributing to the pathogenicity of Acanthamoeba.

3.1. Factors contributing directly to the pathogenicity of Acanthamoeba

3.1.1. Adhesion

Adhesion is an important step in the pathogenic cascades of Acanthamoeba keratitis leading to secondary events and amoebae crossing biological barriers (Fig. 7). Several adhesins have been identified in Acanthamoeba, including a mannose-binding protein [30], a laminin-binding protein with a predicted molecular mass of 28.2 kDa [40] and a 55 kDa laminin-binding protein [87]. Notably, oral immunization with recombinant mannose-binding protein ameliorates Acanthamoeba keratitis in the Chinese hamster model [30, 31], and has shown that the mannose-binding protein gene in Acanthamoeba contains six exons and five introns that span 3.6 kbp. The 2.5 kbp cDNA codes for an 833 amino acids precursor protein with a signal sequence (residues 1–21 aa), an N-terminal extracellular domain (residues 22–733 aa) with five N- and three O-glycosylation sites, a transmembrane domain (residues 734–755 aa), and a C-terminal intracellular domain (residues 756–833 aa).

thumbnail Figure 7.

Schematics of Acanthamoeba-mediated corneal damage. “Blast” refers to damage.

On the host side, parasite binding to specific host cell receptor(s) remains incompletely understood. However Toll-like receptor-4 (TLR-4) is shown to provide a docking site for Acanthamoeba [82, 83]. Complete identification of adhesins involved in binding to various cell types, tissues and surfaces together with specific receptor(s) is a largely unexplored area, offering tremendous research opportunities. The binding of Acanthamoeba to host cells interferes with the host intracellular signalling pathways. For example, TLR activation leads to TLR4-Myeloid differentiation primary response gene 88 (MyD88)-Nuclear Factor-Kappa B (NF-kappaB) and TLR4-Extracellular signal-regulated kinases1/2 (ERK1/2) pathways [82, 83]. This was confirmed using anti-TLR antibodies or specific inhibitors pyrrolidinedithiocarbamate (PDTC) (for the NF-kappa B pathway) and U0126 (for the ERK pathway). Using cell cycle microarrays, it has been shown that adhesion of Acanthamoeba to host cells regulates the expression of a number of genes important for the cell cycle such as GADD45A and p130 Rb, associated with cell cycle arrest, as well as inhibiting the expression of other genes, such as those for cyclins F, G1 and cyclin dependent kinase-6 that encode proteins important for cell cycle progression [95]. Acanthamoeba inhibited pRb phosphorylation (a master regulator of cell cycle) in human corneal epithelial cells, indicating that Acanthamoeba induces cell cycle arrest in the host cells. Acanthamoeba-mediated host cell death is dependent on the activation of phosphatidylinositol 3-kinase [96]. This was shown using LY294002, a specific phosphatidylinositol 3-kinase inhibitor, which blocked Acanthamoeba-mediated host cell death. These findings were further confirmed using host cells expressing dominant negative p85, i.e. a regulatory subunit of phosphatidylinositol 3-kinase. The host cells expressing dominant negative phosphatidylinositol 3-kinase were significantly less susceptible to Acanthamoeba-mediated damage (Fig. 8). Chusattayanond et al. [16] have shown that host cell apoptosis induced by Acanthamoeba is caspase-dependent, mediated by over-expression of pro-apoptotic proteins in the mitochondrial pathway, while Tripathi et al. [102] demonstrated the role of the cytosolic phospholipase A2α (cPLA2α) pathway in host cell apoptosis.

thumbnail Figure 8.

Acanthamoeba-mediated corneal epithelial cell death.

3.1.2. Phagocytosis

Adhesion of Acanthamoeba leads to secondary processes such as phagocytosis or secretion of toxins. The primary role of Acanthamoeba phagocytosis is to take up food particles. However, the ability of Acanthamoeba to form food cups or amoebastomes during incubations with the host cells suggests it has a role in the pathogenesis of Acanthamoeba [26, 47, 76]. Within 40 s, bound particles are surrounded by pseudopods, brought into the cytoplasm, and released as phagosome into the cytoplasmic stream. The oxidative metabolism in Acanthamoeba has some remarkable similarities to the respiratory burst oxidase of neutrophils [13]. Cytochalasin D, an inhibitor of actin polymerization blocked Acanthamoeba-mediated host cell death, confirming that actin-mediated cytoskeletal rearrangements play an important role in the pathogenesis of Acanthamoeba [70, 100]. Genistein (a protein tyrosine kinase inhibitor) inhibited, while sodium orthovanadate (protein tyrosine phosphatase inhibitor), stimulated Acanthamoeba phagocytosis, indicating that tyrosine kinase-induced actin polymerization is important in Acanthamoeba phagocytosis [3]. Rho kinase inhibitor, Y27632, partially blocked Acanthamoeba phagocytosis. Y27632 is known to block stress fibre formation by inhibiting myosin light chain phosphorylation and cofilin phosphorylations but independent of the profilin pathway. LY294002, a specific inhibitor of phosphatidylinositol 3-kinase, inhibited Acanthamoeba phagocytosis. Inhibition of Src kinase using a specific inhibitor, PP2 (4-amino-5-(4 chlorophenyl)-7-(t-butyl)pyrazolo [3,4-d] pyrimidine) but not its inactive analog, PP3 (4-amino-7-phenylpyrazolo[3,4-d] pyrimidine), hampered the phagocytic ability of A. castellanii [93]. The precise elucidation of molecular mechanisms associated with Acanthamoeba phagocytic pathways will be of value in the development of therapeutic interventions.

3.1.3. Ecto-ATPases

Ecto-ATPases are glycoproteins expressed in the plasma membranes with their active sites facing the external medium. Ecto-ATPases hydrolyze extracellular ATP and other nucleoside triphosphates. The resultant ADP can have toxic effects on the host cells. For example, it has been shown that ADP released by Acanthamoeba bind to P2y2 purinergic receptors on the host cells, causing an increase in intracellular calcium, inducing caspase-3 activation and finally resulting in apoptosis [59]. A P2 receptor antagonist, suramin, inhibited Acanthamoeba-mediated host cell death [59], suggesting that ecto-ATPases play an important role in Acanthamoeba pathogenesis in a contact-independent mechanism. The clinical isolates of Acanthamoeba exhibited higher ecto-ATPase activities compared with weak pathogenic isolates [94]. Several ecto-ATPases of approximate molecular weights of 62, 100, 218, 272 and more than 300 kDa have been described in Acanthamoeba. However, further research is needed to elucidate their function in Acanthamoeba biology, and investigate their precise role in Acanthamoeba pathogenesis.

3.1.4. Neuraminidase activity

Acanthamoeba exhibited neuraminidase activity. The enzyme activity is optimal at pH 5 and at temperatures of 25–30 °C. The live amoebae released sialic acid from the human cells. Therefore, the neuraminidase of Acanthamoeba could be relevant in the colonization of amoebae, and important in producing damage of the sialic acid-rich corneal epithelium. Interestingly, neuraminidases of Trypanosoma cruzi and Acanthamoeba are immunologically related, as demonstrated by antibodies against neuraminidase of Trypanosoma cruzi, which reacted with Acanthamoeba in immunofluorescence, immunoblotting and enzyme-linked immunosorbent assays [73, 74].

3.1.5. Superoxide dismutase

The enzyme superoxide dismutase catalyzes the dismutation of superoxide into oxygen and hydrogen peroxide. It is an important antioxidant defence exposed to oxygen. Superoxide is one of the main reactive oxygen species in the cell and as such, superoxide dismutase plays an important antioxidant role. Two superoxide dismutases have been identified in Acanthamoeba: an iron superoxide dismutase (approximate molecular weight of 50 kDa) and a copper-zinc superoxide dismutase (approximate molecular weight of 38 kDa). These enzymes occur as cytoplasmic and detergent-extractable fractions. They may be potential virulence factors of Acanthamoeba by acting both as anti-oxidants and anti-inflammatory agents. They may also provide additional targets for chemotherapy and immuno-diagnosis of Acanthamoeba infections [15]. A. castellanii iron superoxide dismutase may play essential roles in the survival of amoebae not only by protecting themselves from endogenous oxidative stress, but also by detoxifying oxidative killing of amoebae by host immune effector cells [50].

3.1.6. Acanthamoeba-induced plasminogen activation

Acanthamoeba displayed plasminogen activator activity by catalyzing the cleavage of host plasminogen to form plasmin, which can activate host proteolytic enzymes, such as pro-matrix metalloproteases. Once activated, the matrix metalloproteases degrade the basement membranes and the components of the extracellular matrix such as type I and type II collagens, fibronectins and laminin. Thus, the matrix metalloproteinases are involved in tissue remodelling. The pathogenic Acanthamoeba showed positive chemotactic response to the endothelial extracts [109].

3.1.7. Elastase

Acanthamoeba is known to produce elastase with broad specificity. Moreover, elastases are known to degrade a range of connective tissue proteins such as elastin, an elastic fibre, fibrinogen, collagen, and proteoglycans, which together determined the mechanical properties of the connective tissue. Tissues altered by prior elastase treatment are more susceptible to oxygen radical attack, suggesting their involvement in the pathogenesis and pathophysiology of Acanthamoeba infections [18, 46, 47, 54]. The elastases were in the region of 70–130 kDa and serine peptidases were found to be possible elastase candidates [28].

3.1.8. Proteases

Proteases are degradative enzymes that catalyze the total hydrolysis of proteins. Acanthamoeba is shown to exhibits proteolytic activities. The primary role of Acanthamoeba proteases is to degrade food substances for feeding purposes. Pathogenic Acanthamoeba exhibit increased extracellular protease activities. The link between pathogenicity and the increased levels of extracellular proteases suggests that pathogenic Acanthamoeba utilize proteases to facilitate invasion of the host. Acanthamoeba is known to produce serine, cysteine and metalloproteases. Several serine proteases have been identified ranging in molecular weights from >20 kDa to >200 kDa. They are shown to possess collagen degradation activity, plasminogen activator, and degradation of fibronectin, fibrinogen, IgG, IgA, albumin, haemoglobin, protease inhibitors, interleukin-1, chemokines and cytokines [46, 54, 55, 60]. A 133 kDa serine protease, called MIP133 has been identified as a crucial component of the pathogenic cascade of Acanthamoeba pathogenesis. The MIP133 serine protease is shown to induce the degradation of keratocytes, iris ciliary body cells, retinal pigment epithelial cells, corneal epithelial cells and corneal endothelial cells, and induce apoptosis in macrophage-like cells. The properties of serine proteases facilitate Acanthamoeba invasion of the corneal stroma, leading to secondary reactions such as oedema, necrosis and inflammatory responses. A direct functional role of serine proteases in Acanthamoeba infections is indicated by the observations that intrastromal injections of Acanthamoeba conditioned medium produced corneal lesions in vivo, similar to those observed in Acanthamoeba keratitis patients, and this effect is inhibited by phenylmethylsulfonyl fluoride, a serine protease inhibitor [37, 67, 68]. In addition, the chemically synthesized siRNA against the catalytic domain of the extracellular serine proteases of Acanthamoeba reduced protease activity and Acanthamoeba-mediated host cell cytotoxicity. These results support the idea that extracellular serine proteases are directly involved in the pathogenesis and virulence of Acanthamoeba [55]. In addition, several cysteine proteases have been identified in Acanthamoeba, including 43, 65, 70 and 130 kDa cysteine proteases [46, 47]. In addition to serine and cysteine proteases, there is evidence for metalloprotease activity in Acanthamoeba. An 80 kDa metalloprotease was identified in co-cultures of Acanthamoeba and host cells, but its origin (whether Acanthamoeba or the host cells) was not established. Later studies identified a 150 kDa extracellular metalloprotease from Acanthamoeba isolate of the T1 genotype. This metalloprotease exhibited properties of extracellular matrix degradation, as demonstrated by its activity against collagen I and III (major components of the collagenous extracellular matrix), elastin (elastic fibrils of the extracellular matrix), plasminogen (involved in proteolytic degradation of the extracellular matrix), as well as degradation of casein, gelatine and haemoglobin.

Recently, the complete sequence of a type-1 metacaspase from Acanthamoeba was reported, comprising 478 amino acids [102]. Later studies revealed that A. castellanii metacaspases associate with the contractile vacuole and have an essential role in cell osmoregulation suggesting its attractiveness as a possible target for treatment therapies against A. castellanii infection [89]. These studies showed that Acanthamoeba exhibited diverse proteases and elastases, which could play important roles in Acanthamoeba infections. The precise mechanisms of protease mode of action at the molecular level are only beginning to emerge. Proteases have been shown to be “druggable” targets, as evidenced by the widespread use of protease inhibitors as effective therapy for hypertension and AIDS, and the current clinical development of protease inhibitors for diabetes, cancer, thrombosis, and osteoporosis. As long as issues such as the difficulty of achieving selectivity can be addressed through targeting allosteric sites, protease-based drug therapy has tremendous potential in the treatment of many infectious diseases. Future studies will further determine the role of proteases as vaccine targets, search for novel inhibitors by screening of chemical libraries, or rational development of drugs based on structural studies should enhance our ability to target these important pathogens.

3.1.9. Phospholipases

During phagocytosis, there is a large turnover of the plasma membrane in Acanthamoeba, indicating that there is controlled local degradation of phospholipids leading to instability of the membrane phospholipid bilayer, which would then reform after the acylation of the lysophospholipid. In support of this, all of the enzymes that are needed for such a cycle are present in the plasma membrane of Acanthamoeba, including phospholipase A2, acyl CoA:lysolecithin acyltransferase, and acyl CoA synthetase. Phospholipase A1 and lysophospholipase are also present in the plasma membrane of Acanthamoeba. The plasma membrane lysophospholipase may also serve to protect the cell from the lytic effect of lysophospholipids either of exogenous or endogenous origin. The plasma membranes have the enzymatic capability of modulating the fatty acyl composition of phospholipids by de-acylation and acylation. Our knowledge of phospholipases in the virulence of Acanthamoeba is fragmented, however several studies have shown that pathogenic Acanthamoeba that exhibit cytopathic effects on mammalian cells in vitro liberate more phospholipase, suggesting their possible involvement in Acanthamoeba infections. Because phospholipases cleave phospholipids, it is reasonable to suspect that they play a role in membrane disruptions, penetration of host cells, and cell lysis. However this remains to be determined. Other actions of phospholipases may involve interference with intracellular signalling pathways. Phospholipases generate lipids and lipid-derived products that act as second messengers. A. castellanii lysates and their conditioned medium exhibited phospholipase activities [66]. Sphinganine, a PLA2 inhibitor showed robust amoebistatic properties but had no effect on the viability of A. castellanii. These studies suggest that Acanthamoeba phospholipases and/or lysophospholipases may play a role in producing host cell damage or affect other cellular functions such as induction of inflammatory responses, thus facilitating Acanthamoeba virulence. More studies are needed to identify and characterize Acanthamoeba phospholipases and to determine their potential role in the development of therapeutic intervention. This is not a novel concept: earlier studies have shown that phospholipase C from Clostridium perfringens induced protection against C. perfringens-mediated gas gangrene. In addition, targeting of phospholipases using synthetic inhibitor compounds has been shown to prevent Candida infections. Antibodies produced against Acanthamoeba phospholipases may also be of potential value in the development of sensitive and specific diagnostic assays as well as of therapeutic value [42].

3.1.10. Glycosidases (also called glycoside hydrolases)

Glycoside hydrolases catalyze the hydrolysis of glycosidic linkage to generate smaller sugars. Glycoside hydrolases are ubiquitous in nature and involved in the degradation of biomass such as cellulose and in a variety of cellular functions. Together with glycosyltransferases, glycosidases form the major catalytic machinery for the synthesis and breakage of glycosidic bonds. Acanthamoeba exhibits glycosidase activities including beta-glycosidase, alpha-glucosidase, beta-galactosidase, beta-N-acetyl-glucosaminidase, beta-N-acetyl-galactosaminidase and alpha-mannosidase [38, 39]. Acanthamoeba extracts mediate enzymatic lysis of cell walls from several species of bacteria including Micrococcus lysodeikticus, Micrococcus roseus, Streptococcus faecalis, Bacillus megaterium, Sarcina lutea, Micrococcus radiodurans and limited activity against Bacillus subtilis, Bacillus cereus, but has no effects on Acanthamoeba cyst walls or chitin. Exhaustive digestion of Micrococcus lysodeikticus cell walls released free N-acetyl-glucosamine, N-acetyl-muramic acid, glycine, alanine, glutamic acid and lysine, suggesting that Acanthamoeba possesses both endo- and exo-hexosaminidases and beta-N-acetyl-hexosaminidases. Since Acanthamoeba is known to utilize maltose, cellobiose, sucrose or lactose, some of the glycosidases indicated above may suggest the utilization of these disaccharides [42].

3.1.11. Acanthaporin

Recently, acanthaporin, the first pore-forming toxin was described from Acanthamoeba [64]. Acanthaporin was isolated from extracts of virulent A. culbertsoni by tracking its pore-forming activity, molecularly cloning the gene of its precursor, and recombinant expression of the mature protein in bacteria. Acanthaporin was cytotoxic for human neuronal cells and exerted antimicrobial activity against a variety of bacterial strains by permeabilizing their membranes [64]. The tertiary structures of acanthaporin’s active monomeric form and inactive dimeric form, both solved by NMR spectroscopy, revealed a currently unknown protein fold and a pH-dependent trigger mechanism of activation.

3.2. Factors contributing indirectly to Acanthamoeba pathogenicity

The ability of Acanthamoeba to produce human diseases is a multifactorial process and is, amongst other factors, dependent on its ability to survive outside its host and under diverse conditions (high osmolarity, varying temperatures, food deprivation and resistance to chemotherapeutic drugs) [24, 48, 106, 107, 114]. The ability of Acanthamoeba to overcome such conditions can be considered as contributory factors towards disease and are indicated below.

3.2.1. Morphological features

The infective forms of Acanthamoeba or trophozoites do not have a distinct morphology. However, they do possess spine-like structures known as acanthopodia on their surface, which allow them to modulate binding of Acanthamoeba to biological and inert surfaces. In addition, their amoeboid motion resembles that of macrophages/neutrophils and it is likely that Acanthamoeba employ similar strategies to traverse biological barriers and invade tissues using the paracellular route.

3.2.2. Temperature tolerance, osmotolerance and growth at different pH

Being a free-living amoeba, Acanthamoeba is exposed to various temperatures, osmolarity and pH. Similarly contact with tear film exposes Acanthamoeba to high osmolarity (due to salinity in tears), high temperatures as well as alterations in pH. For successful transmission, Acanthamoeba must withstand such stress and exhibit biological activity. Pathogenic Acanthamoeba showed high levels of heat shock proteins (i.e. HSP60 and HSP70) compared with weak pathogens [75, 77]. The higher levels of heat shock proteins in Acanthamoeba may indicate their involvement in (i) tolerance to hosts’ stressors and/or (ii) in species’ virulence [75]. The ability of Acanthamoeba to grow at high temperatures and high osmolarity correlates with the pathogenicity of Acanthamoeba isolates, and may provide a good indicator of the pathogenic potential of a given isolate [46, 47, 54]. The precise mechanisms by which pathogenic Acanthamoeba adapt to higher temperatures and maintain their metabolic activities require further studies.

3.2.3. Cellular differentiation

Cellular differentiation is the ability of Acanthamoeba to differentiate into a morphologically distinct dormant cyst form or a vegetative trophozoite form. This is a reversible change, dependent on environmental conditions. Cysts are resistant to various antimicrobial agents and adverse conditions such as extremes in temperatures, pH, osmolarity, desiccation and cysts can be airborne: all of which presents a major problem in chemotherapy because their persistence may lead to recurrence of the disease. Furthermore, Acanthamoeba cysts can survive several years while maintaining their pathogenicity [62]. These characteristics suggested that the primary functions of cysts lie in withstanding adverse conditions and in the spread of amoebae throughout the environment. In addition, this may represent the ability of Acanthamoeba to alternate expression of surface proteins/glycoproteins, in response to changing environments and/or immune surveillance. Cellular differentiation represents a major factor in the transmission of Acanthamoeba and recurrence of its infection. However, the underlying molecular mechanisms in these processes remain incompletely understood and warrant further investigation.

3.2.4. Chemotaxis

Chemotaxis directs amoeba movement according to certain chemicals in their environment. This is important as Acanthamoeba moves towards the highest concentration of food molecules, or to flee from poisons. Acanthamoeba exhibits chemosensory responses as observed by their response to a variety of bacterial products or potential bacterial products by moving actively towards the attractant. Acanthamoeba responded to the chemotactic peptides formyl-methionyl-leucyl-phenylalanine, formyl-methionyl-leucyl-phenylalaninebenzylamide, lipopolysaccharide and lipid A. In addition, significant responses to cyclic AMP, lipoteichoic acid and N-acetyl-glucosamine were also found. Interestingly, chemotactic peptide antagonists, mannose, mannosylated bovine serum albumin and N-acetyl-muramic acid all yielded non-significant responses. Pretreatment of Acanthamoeba with chemotactic peptides, bacterial products and bacteria reduced the directional response to attractants. Acanthamoeba grown in the presence of bacteria appeared more responsive to chemotactic peptides. Treatment of Acanthamoeba with trypsin reduced the response of cells to chemotactic peptides, though sensitivity was restored within a couple of hours [7, 92]. These findings suggest that Acanthamoeba membranes possess receptors sensitive to these bacterial substances, which are different from the mannose-binding protein involved in binding to the host cells to produce cytotoxicity or involved in binding to bacteria during phagocytosis. The rate of movement is relatively constant (ca. 0.40 μm per sec), indicating that the locomotor response to these signals is a taxis, or possibly a klinokinesis, but not an orthokinesis [92].

3.2.5. Ubiquity

Acanthamoeba has been found in diverse environments, from drinking water to distilled water wash bottles, deep ocean bottom and Antarctica. It is therefore not surprising that human beings encounter and interact regularly with these organisms, as is evidenced by findings that in some regions, up to 100% of the population tested possess Acanthamoeba antibodies, suggesting that these are one of the most ubiquitous protists and often come into contact with human beings, and given the opportunity (e.g. contact lens wear), can cause serious infections.

3.2.6. Biofilms

Biofilms are known to play an important role in the pathogenesis of Acanthamoeba keratitis. Biofilms are microbially-derived sessile communities, which can be formed in aqueous environments as well as on any materials and medical devices including intravenous catheters, contact lenses, scleral buckles, suture material, and intraocular lenses. In the instance of contact lenses, biofilms are formed through contamination of the storage case. Once established, biofilms provide attractive niches for Acanthamoeba by fulfilling their nutritional requirements as well as providing resistance to disinfectants. In addition, this allows higher binding of Acanthamoeba to contact lenses. For example, Acanthamoeba exhibits significantly higher binding to used and Pseudomonas biofilm-coated hydrogel lenses compared to unworn contact lenses. The abundant nutrient provided by the biofilm encourages transformation of Acanthamoeba into the vegetative, infective trophozoite form, and it is important to remember that binding of Acanthamoeba to the human corneal epithelial cells most likely occurs during the trophozoite stage as cysts exhibit minimal binding. These findings suggest that biofilms play an important role in Acanthamoeba keratitis in wearers of contact lenses and preventing biofilm formation is perhaps an important preventative strategy [9, 118].

3.2.7. Host factors

The factors that enable Acanthamoeba to produce disease are not limited solely to the pathogen, but most likely involve host determinants [17, 115]. Evidence for this comes from recent studies in the UK, Japan and New Zealand, which suggested that the storage cases of contact lenses of 400–800 per 10,000 asymptomatic wearers are contaminated with Acanthamoeba. This number is remarkably high compared with the incidence rate of Acanthamoeba keratitis in wearers of contact lenses, which is around 0.01–1.49 per 10,000 [46]. These findings suggest that factors such as host susceptibility, tissue specificity, tear factors, sIgA, corneal trauma, as well as environmental factors such as osmolarity may be important in initiating Acanthamoeba infections. However, the extent to which such host factors contribute to the outcome of Acanthamoeba keratitis is unclear because host factors are more complex and difficult to study than those of the pathogen. Overall, it can be concluded that Acanthamoeba traversal of biological barriers and to produce disease is a complex process that involves both pathogen as well as host factors.

4. Acanthamoeba keratitis treatment: a problem with no simple solution?

The treatment of Acanthamoeba keratitis has evolved since the first medical cure was reported in 1985 [46, 54, 86, 103106, 111, 112]. Early diagnosis and aggressive medical therapy has improved the management of this difficult infection. Other reported factors that may facilitate effective medical therapy and an improved outcome include early epithelial debridement (to remove the majority of organisms) and penetrating keratoplasty in medically-resistant cases.

So far, no chemotherapeutic agent has been described as a single effective treatment against AK, regardless of the isolate or genotype that causes it. This is because there are many factors, including the wide range of virulence traits that different isolates possess, which makes it almost impossible to establish a correlation between in vitro and in vivo efficacies. Nevertheless, to establish the most effective treatment regimen is not easy for several reasons such as the relatively small number of reported cases of AK, variable pathogenicity of different strains, and the intrinsic fluctuating nature of the disease process.

4.1. Is there a single effective treatment against AK?

There are currently no methods or a single drug that can eliminate both cystic and trophozoite forms, while the trophozoite form is much more readily eliminated [46, 47, 54, 56].

The available reported treatment regimens in the literature have varied widely depending on the manifestation of the disease, the general health status of the infected cornea, and the experience of the clinician. For example, in the original AK case reported by Naginton et al. [reviewed in 46, 54], numerous topical antimicrobial preparations were tried in conjunction with steroids, but both eyes eventually required grafting. Recent years have brought us knowledge of more specific antimicrobials, although unfortunately, surgical grafting of the cornea remains the last solution in case of severe infection.

4.2. Current therapeutic approaches

Current AK treatment consists of topical antimicrobial agents, which can achieve high concentrations at the site of infection. Moreover, due to the existence of a cyst form in Acanthamoeba that is highly resistant to therapy, a combination of agents is generally used.

Most of the currently used topical agents are effective against trophozoites and cysts of Acanthamoeba such as biguanides, (i) PHMB [52, 54, 58], which is effective at low concentrations (0.02%), but is unfortunately toxic to human corneal cells [52, 54], and (ii) chlorhexidine, which is effective against both amoebic forms, and at minimal concentrations is not toxic to corneal epithelial cells [52, 54, 58, 86]. Chlorhexidine 0.02% is often used in combination with aromatic diamidines such as 0.1% propamidine isethionate Brolene® (Sanofi, UK), 0.15% dibromopropamidine, hexamidine 0.1% Desomedine© (Chauvin, France) and neomycin, showing good results if the treatment is applied early in the development of the infection [54, 86]. Unfortunately, propamidine and hexamidine are not available in all countries.

These topical antimicrobials are administered every hour immediately after corneal debridement or for the first several days of therapy. These agents are then continued hourly for 3 days (at least nine times/day is recommended) depending on clinical response. The frequency is then reduced to every 3 h. Two weeks may be required before a response is observed, and the total duration of therapy is a minimum of 3–4 weeks. Some authors also recommend treatment for 6–12 months. Moreover, when therapy is discontinued, close observation of the patient is suggested in order to avoid recurrent infection. Some patients have been successfully treated using an antiseptic as monotherapy; if this is attempted, it should be reserved for patients with early disease.

4.3. Biguanides as first line treatment against AK

PHMB and chlorhexidine have been reported to be the most effective drugs for treatment of infection and in combination they have been reported to be effective against both cysts and trophozoites [23, 52, 54, 79, 108]. Regarding these two drugs, it is important to mention that they are active against a wide spectrum of pathogens by increasing cytoplasmic membrane permeability. Chlorhexidine and PHMB both contain highly charged positive molecules capable of binding to the mucopolysaccharide plug of the ostiole resulting in penetration of the amoeba. The drug then binds to the phospholipid bilayer of the cell membrane which is negatively charged resulting in damage, cell lysis and death [52].

Among the observed side effects, toxic keratopathy may develop at any time, necessitating significant alteration in this treatment plan [46, 54, 98]. Elevated intraocular pressure as well as increased inflammation often requires the use of antiglaucoma medication and cycloplegics. The role of topical corticosteroids as well as surgical intervention with therapeutic penetrating keratoplasty in the management of this infection remains controversial and is discussed later.

Brolene® may be accompanied by drug toxicity and resistance and topical treatment with miconazole can lead to epithelial toxicity [29, 54, 56]. According to Turner et al. [107], resistance is mainly due to the exocyst and endocyst, which forms a double-walled protective barrier to biocides. Cysts may also be resistant to biocides because they show little or no metabolic activity and because of selection pressure due to continuous drug exposure [46, 106, 107]. If resistance to drugs occurs, keratoplasty may be used [29, 46, 51, 54]. Ueki et al. [108] stated that recommended treatment for AK includes corneal scrape with antifungal drugs and antibiotic treatment. However, antifungal, antibacterial, antiviral and even corticosteroids used can complicate matters because they cause initial improvement then worsening of the disease [46, 54].

4.4. Steroids controversy in AK treatment

No clear consensus exists about use of steroids. Most authorities recommend that steroid use is probably best avoided. Patients receiving steroids should continue antiamoebic therapy for several weeks after the steroids are stopped. In the case of a persistent infection with inflammation, corticosteroids may be used. However, their use is controversial because they cause suppression of the immunological response of the patient. Moreover, corticosteroids produce inhibition of the processes of encystation and excystation of Acanthamoeba, which could be a cause of the appearance of resistance problems [103]. Recent studies have highlighted an association of topical corticosteroids and a diagnostic delay of AK. Moreover, there is some evidence that suggests that steroid use may result in increased pathogenicity of the amoebae [85]. McClellan et al. [63] demonstrated in an in vivo model that the addition of topical corticosteroids, even at low doses, promotes an increase in the number of trophozoites, produced by excystment in the infected corneal stroma. This exposes patients to the risk of significantly greater corneal destruction through an increase in amoebic load, which may be greater than the increased chemotherapy effect on trophozoites compared with the more resistant cysts [63, 85].

Furthermore, corneal transplantation (keratoplasty) is another therapeutic option when topical treatment has failed. This intervention is recommended if in the acute phase of infection, the cornea becomes too thin or has been damaged, and vision is limited [51, 69]. Nevertheless, there is a risk of not eliminating all the trophozoites or cysts that could colonize the new cornea [98]. A variation of keratoplasty called DALK (Deep Anterior Lamellar Keratoplasty) has been proposed to be more effective in increasing the survival of transplanted corneal cells and to prevent entry of pathogenic organisms at the time of surgery [72].

4.5. In vitro drug sensitivity testing and personalised treatments in AK patients

In vitro drug sensitivity testing, although rarely used, may be helpful in refractory cases. However, such testing has its limitations and may not be practical for the clinician. Not only may drug sensitivities be variable between strains, but a strain may also become resistant to formerly effective drugs. In addition, testing results may differ between laboratories and in some cases may not correlate with the clinical course. Despite these problems, drug sensitivity testing may offer the clinician a small edge in improving chances of therapeutic success and should be employed when possible. Recently, a patient suffering from severe AK was healed after a personalized treatment with voriconazole, when sensitivity to this drug was assayed after isolation of the amoebae from the patient’s cornea [5].

4.6. Surgical management of AK

Therapeutic penetrating keratoplasty was the mainstay of treatment for AK before the development of early diagnosis and aggressive medical therapy [10, 21, 36, 72]. The role and timing of penetrating keratoplasty in AK still remains poorly defined. Certainly pending or frank corneal perforation is a clear indication for surgical intervention. However, other indications for surgery are not well defined.

Therapeutic penetrating keratoplasty should be considered when the infectious process spreads to the paracentral corneal stroma despite maximum antiamoebic therapy [21]. Performing this procedure on a more localized infection may allow total removal of the organisms by excising the clinically involved tissue as well as a rim of clear surrounding cornea. This procedure allows the donor tissue to be placed into a relatively undamaged and hence non-immunocompromised recipient bed. After surgery, medical therapy should be continued for at least several months to help ensure elimination of any residual Acanthamoeba organisms in the recipient stromal tissue. Once the infection has spread into the peripheral cornea, however, the likelihood of achieving a surgical cure is markedly diminished. Intensive medical management is required for several months to eradicate the organism prior to keratoplasty. Unfortunately, the prognosis in these cases is poor and reinforces the rationale for earlier rather than later surgical treatment.

Recently, bipedicle conjunctival flap (CF) and cryopreserved amniotic membrane graft (AMG) have been reported to be effective in AK. They restore ocular surface integrity and provide metabolic and mechanical support for corneal healing. Nevertheless, in the case of large corneal perforation, penetrating keratoplasty to restore ocular integrity remains as the only effective surgical option [1].

4.7. Novel therapeutic approaches

Recently, the widespread use of photorefractive surgery has inspired its use in the setting of AK. Kandori et al. [44] reported four cases in 2010, where early stage AK was treated with standard topical therapy, but developed large corneal abscesses in the upper third thickness of the stroma. These were removed using laser phototherapeutic keratectomy (PTK); all eyes experienced no disease recurrence and final acuities ranged from 20/16 to 20/25.

Cross-linking is another relatively new treatment option that has been applied to AK. While in vitro studies by Kashiwabuchi et al. [45] and Del Buey et al. [25] have shown no amoebicidal effect of riboflavin combined with UVA exposure, clinical case reports have shown a much more promising picture. Garduño-Vieyra et al. [32] administered collagen cross-linking to a patient in Mexico instead of topical medical therapies, which were not commercially available. Significant improvement was observed after 24 h, with symptoms resolving within 3 months, and 20/20 vision was obtained after 5 months. Khan et al. [49] have since reported three similar cases which responded equally well to cross-linking, with all ulcers closing within 7 weeks. In subsequent PK surgery for scarring, no organisms were detected in excised tissue. It is possible that the collagen stabilizing effect prevents further tissue damage and isolates and prevents reproduction of the amoebae. Although individual case report results seem promising, there are no formal clinical trials thus far to recommend incorporation into standard practice.

4.8. In the search of novel drugs against AK

A new path may be the application of alkylphosphocholines. These are phosphocholines esterified to aliphatic alcohols. They exhibit in vitro and in vivo antineoplastic activity and have been shown to be cytotoxic against Leishmania spp., Trypanosoma cruzi and Entamoeba histolytica. A recent study has demonstrated that particularly hexadecylphosphocholine (miltefosine) is highly effective also against various strains of Acanthamoeba. Moreover, it has recently been applied in combination with PHMB in AK in Austria with successful outcomes [8, 78, 79].

Recently, the creation of a “pharmaceutical phylogeny” has been started for Acanthamoeba in order to elucidate and select new therapeutic targets [54, 58, 86]. The phylogeny of Acanthamoeba is closer evolutionarily to human beings than many other eukaryotic pathogens [69]. Therefore, part of the hypothesis is that many biochemical processes as well as therapeutic targets are evolutionarily conserved and are similar in related organisms. This implies that there will be a large number of processes, some still unknown, in Acanthamoeba that are similar to those of human beings. Therefore, treatments that affect the host could also affect the parasite, for example, phospholipid analogues as mentioned above which have been demonstrated to be effective against Acanthamoeba [2, 86]. However, even though many biological processes are similar in Acanthamoeba to other eukaryotic cells, some proteins such as tubulins are not sensitive to inhibitors that are normally used against them [86]. Therefore, it is also interesting to find those targets that are specific to Acanthamoeba in order to attack the parasite without affecting the host. These targets may be of a different nature: specific gene products, biological processes themselves, transcription or translation mechanisms or physical attributes such as cell membranes. In addition, many antibiotics active against Acanthamoeba have a mechanism of action which is still unknown. In recent years, the possibility to design and synthesize specific small interfering RNAs (siRNAs) for gene silencing have made RNAi techniques a powerful tool for the study and understanding of new cellular pathways of proteins whose functions are still unknown, as well as for their use as a therapy against various diseases [14, 88]. In the case of Acanthamoeba, siRNAs have been used successfully to identify potential therapeutic targets and even recently to establish a target and propose statins as a future therapy against Acanthamoeba strains [58].

Other drug targets that have been validated using the same approach, but without the elucidation of an available chemical alternative (active principle/drug) include glycogen phosphorylase and other cellulose synthesis related enzymes, serine proteases and myosin IC [4, 27, 53, 55, 57, 65]. The recently published Acanthamoeba castellani genome data will further assist in the development of novel therapeutics in the near future [19].

5. Concluding remarks

The number of reported cases of Acanthamoeba keratitis is increasing worldwide every year, due to increasing contact lens use for vision correction and cosmetic purposes. Increased awareness combined with early diagnosis of the disease is currently a good pathway towards better outcomes. However, knowledge about the pathogenesis and cellular differentiation processes in Acanthamoeba are still not fully known and urgently require further investigation. They hold the key to improved diagnosis and to development of effective therapeutic approaches.

Acknowledgments

JLM was supported by the Ramón y Cajal Subprogramme from the Spanish Ministry of Economy and Competitivity RYC-2011-08863 and by the grants RICET (Project No. RD12/0018/0012 of the programme of Redes Temáticas de Investigación Cooperativa, FIS), Spanish Ministry of Health, Madrid, Spain and the Project FIS PI13/00490 “Protozoosis Emergentes por Amebas de Vida Libre: Aislamiento, Caracterización, Nuevas Aproximaciones Terapéuticas y Traslación Clínica de los Resultados” from the Instituto de Salud Carlos III and Project ref. AGUA3 “Amebas de Vida Libre como Marcadores de Calidad del Agua” from CajaCanarias Fundación. JLM is grateful to the laboratory members of the Free-Living Amoebae Laboratory at the University Institute of Tropical Diseases and Public Health of the Canary Islands, University of La Laguna, Spain.

NAK was supported by the Higher Education Commission, and Aga Khan University, Pakistan, the British Council for the Prevention of Blindness, UK, and the Royal Society, UK.

JW was supported by the Medical University of Vienna, Austria and would like to thank all members of the Molecular Parasitology laboratory at the Institute of Specific Prophylaxis and Tropical Medicine, Vienna, Austria.

This review was invited by the Editor at the occasion of ICOPA XIII (Mexico, 2014). Its publication is sponsored by the publisher of Parasite, EDP Sciences.

Images from Figure 1 were kindly provided by Dr Francisco Arnalich-Montiel, Cornea Unit, Hospital Ramón y Cajal, Madrid, Spain.

References

  1. Abdulhalim B, Wagih MM, Gad AA, Boghdadi G, Nagy RR. 2015. Amniotic membrane graft to conjunctival flap in treatment of non-viral resistant infectious keratitis: a randomised clinical study. British Journal of Ophthalmology, 99(1), 59–63. [CrossRef] (In the text)
  2. Aichelburg AC, Walochnik J, Assadian O, Prosch H, Steuer A, Perneczky G, Visvesvara GS, Aspöck H, Vetter N. 2008. Successful treatment of disseminated Acanthamoeba sp. infection with miltefosine. Emerging Infectious Diseases, 14, 1743–1746. [CrossRef] [PubMed] (In the text)
  3. Alsam S, Sissons J, Dudley R, Khan NA. 2005. Mechanisms associated with Acanthamoeba castellanii (T4) phagocytosis. Parasitology Research, 96, 402–409. [CrossRef] [PubMed] (In the text)
  4. Aqeel Y, Siddiqui R, Khan NA. 2013. Silencing of xylose isomerase and cellulose synthase by siRNA inhibits encystation in Acanthamoeba castellanii. Parasitology Research, 112(3), 1221–1227. [CrossRef] [PubMed] (In the text)
  5. Arnalich-Montiel F, Martín-Navarro CM, Alió JL, López-Vélez R, Martínez-Carretero E, Valladares B, Piñero JE, Lorenzo-Morales J. 2012. Successful monitoring and treatment of intraocular dissemination of Acanthamoeba with voriconazole. Archives of Ophthalmology, 130, 1474–1475. [CrossRef] [PubMed] (In the text)
  6. Bacon AS, Frazer DG, Dart JK, Matheson M, Ficker LA, Wright P. 1993. A review of 72 consecutive cases of Acanthamoeba keratitis, 1984–1992. Eye, 7, 719–725. [CrossRef] (In the text)
  7. Bagorda A, Parent CA. 2008. Eukaryotic chemotaxis at a glance. Journal of Cell Science, 121, 2621–2624. [CrossRef] [PubMed] (In the text)
  8. Barisani-Asenbauer T, Walochnik J, Mejdoubi L, Binder S. 2012. Successful management of recurrent Acanthamoeba keratitis using topical and systemic miltefosine. Acta Ophthalmologica, 900, doi: 10.1111/j.1755-3768.2012.F095.x. (In the text)
  9. Beattie TK, Tomlinson A, McFadyen AK, Seal DV, Grimason AM. 2003. Enhanced attachment of Acanthamoeba to extended-wear silicone hydrogel contact lenses: a new risk factor for infection? Ophthalmology, 110, 765–771. [CrossRef] [PubMed] (In the text)
  10. Blackman HJ, Rao NA, Lemp MA, Visvesvara GS. 1984. Acanthamoeba keratitis successfully treated with penetrating keratoplasty: suggested immunogenic mechanisms of action. Cornea, 3, 125. [CrossRef] [PubMed] (In the text)
  11. Booton GC, Joslin CE, Shoff M, Tu EY, Kelly DJ, Fuerst PA. 2009. Genotypic identification of Acanthamoeba sp. isolates associated with an outbreak of Acanthamoeba keratitis. Cornea, 28(6), 673–676. [CrossRef] [PubMed] (In the text)
  12. Bouheraoua N, Gaujoux T, Goldschmidt P, Chaumeil C, Laroche L, Borderie VM. 2013. Prognostic factors associated with the need for surgery in Acanthamoeba keratitis. Cornea, 32, 130–136. [CrossRef] [PubMed] (In the text)
  13. Brooks SE, Schneider DL. 1985. Oxidative metabolism associated with phagocytosis in Acanthamoeba castellanii. Journal of Protozoology, 32, 330–333. [CrossRef] (In the text)
  14. Campochiaro PA. 2006. Potential applications for RNAi to probe pathogenesis and develop new treatments for ocular disorders. Gene Therapy, 13, 559–562. [CrossRef] [PubMed] (In the text)
  15. Cho JH, Na BK, Kim TS, Song CY. 2000. Purification and characterization of an extracellular serine proteinase from Acanthamoeba castellanii. IUBMB Life, 50, 209–214. [CrossRef] [PubMed] (In the text)
  16. Chusattayanond AD, Boonsilp S, Kasisit J, Boonmee A, Warit S. 2010. Thai Acanthamoeba isolate (T4) induced apoptotic death in neuroblastoma cells via the Bax-mediated pathway. Parasitology International, 59, 512–516. [CrossRef] [PubMed] (In the text)
  17. Clarke DW, Niederkorn JY. 2006. The immunobiology of Acanthamoeba keratitis. Microbes and Infection, 8(5), 1400–1405. [CrossRef] (In the text)
  18. Clarke DW, Niederkorn JY. 2006. The pathophysiology of Acanthamoeba keratitis. Trends in Parasitology, 22(4), 175–180. [CrossRef] [PubMed] (In the text)
  19. Clarke M, Lohan AJ, Liu B, Lagkouvardos I, Roy S, Zafar N, Bertelli C, Schilde C, Kianianmomeni A, Bürglin TR, Frech C, Turcotte B, Kopec KO, Synnott JM, Choo C, Paponov I, Finkler A, Heng Tan CS, Hutchins AP, Weinmeier T, Rattei T, Chu JS, Gimenez G, Irimia M, Rigden DJ, Fitzpatrick DA, Lorenzo-Morales J, Bateman A, Chiu CH, Tang P, Hegemann P, Fromm H, Raoult D, Greub G, Miranda-Saavedra D, Chen N, Nash P, Ginger ML, Horn M, Schaap P, Caler L, Loftus BJ. 2013. Genome of Acanthamoeba castellanii highlights extensive lateral gene transfer and early evolution of tyrosine kinase signaling. Genome Biology, 14(2), R11. [CrossRef] [PubMed] (In the text)
  20. Cohen EJ, Buchanan HW, Laughrea PA, Adams CP, Galentine PG, Visvesvara GS, Folberg R, Arentsen JJ, Laibson PR. 1985. Diagnosis and management of Acanthamoeba keratitis. American Journal of Ophthalmology, 100(3), 389–395. [CrossRef] [PubMed] (In the text)
  21. Cohen EJ, Parlato CJ, Arentsen JJ, Genvert GI, Eagle RC Jr, Wieland MR, Laibson PR. 1987. Medical and surgical treatment of Acanthamoeba keratitis. American Journal of Ophthalmology, 103(5), 615–625. [CrossRef] [PubMed] (In the text)
  22. Cursons RTM, Brown TJ. 1978. Use of cell cultures as an indicator of pathogenicity of free-living amoebae. Journal of Clinical Pathology, 31, 1–11. [CrossRef] [PubMed] (In the text)
  23. Dart JK, Saw VP, Kilvington S. 2009. Acanthamoeba keratitis: diagnosis and treatment update 2009. American Journal of Ophthalmology, 148(4), 487–499. [CrossRef] [PubMed] (In the text)
  24. De Jonckheere JF. 1980. Growth characteristics, cytopathic effect in cell culture, and virulence in mice of 36 type strains belonging to 19 different Acanthamoeba spp. Applied and Environmental Microbiology, 39(4), 681–685. [PubMed] (In the text)
  25. Del Buey MA, Cristóbal JA, Casas P, Goñi P, Clavel A, Mínguez E, Lanchares E, García A, Calvo B. 2012. Evaluation of in vitro efficacy of combined riboflavin and ultraviolet a for Acanthamoeba isolates. American Journal of Ophthalmology, 153(3), 399–404. [CrossRef] [PubMed] (In the text)
  26. Diaz J, Osuna A, Rosales MJ, Cifuentes J, Mascaro C. 1991. Sucker-like structures in two strains of Acanthamoeba: scanning electron microscopy study. International Journal of Parasitology, 21, 365–367. [CrossRef] (In the text)
  27. Dudley R, Alsam S, Khan NA. 2007. Cellulose biosynthesis pathway is a potential target in the improved treatment of Acanthamoeba keratitis. Applied Microbiology and Biotechnology, 75(1), 133–140. [CrossRef] [PubMed] (In the text)
  28. Ferreira GA, Magliano AC, Pral EM, Alfieri SC. 2009. Elastase secretion in Acanthamoeba polyphaga. Acta Tropica, 112, 156–163. [CrossRef] [PubMed] (In the text)
  29. Ficker L, Seal D, Warhurst D, Wright P. 1990. Acanthamoeba keratitis-resistance to medical therapy. Eye, 4, 835–838. [CrossRef] (In the text)
  30. Garate M, Cao Z, Bateman E, Panjwani N. 2004. Cloning and characterization of a novel mannose-binding protein of Acanthamoeba. Journal of Biological Chemistry, 279, 29849–29856. [CrossRef] (In the text)
  31. Garate M, Cubillos I, Marchant J, Panjwani N. 2005. Biochemical characterization and functional studies of Acanthamoeba mannose-binding protein. Infection and Immunity, 73, 5775–5781. [CrossRef] [PubMed] (In the text)
  32. Garduño-Vieyra L, González-Sánchez CR, Hernández-Da Mota SE. 2011. Ultraviolet-a light and riboflavin therapy for Acanthamoeba keratitis: a case report. Case Reports in Ophthalmology, 2(2), 291–295. [PubMed] (In the text)
  33. Gast RJ, Ledee DR, Fuerst PA, Byers T. 1996. Subgenus systematics of Acanthamoeba: Four nuclear 18S rDNA sequence types. Journal of Eukaryotic Microbiology, 43, 498–504. [CrossRef] (In the text)
  34. Griffin JL. 1972. Temperature tolerance of pathogenic and nonpathogenic free-living amoebae. Science, 178, 869–870. [CrossRef] [PubMed] (In the text)
  35. Grossniklaus HE, Waring GO 4th, Akor C, Castellano-Sanchez AA, Bennett K. 2003. Evaluation of hematoxylin and eosin and special stains for the detection of Acanthamoeba keratitis in penetrating keratoplasties. American Journal of Ophthalmology, 136(3), 520–526. [CrossRef] [PubMed] (In the text)
  36. Hamburg A, De Jonckheere JF. 1980. Amoebic keratitis. Ophthalmologica, 181, 74. [CrossRef] [PubMed] (In the text)
  37. He YG, Niederkorn JY, McCulley JP, Stewart GL, Meyer DR, Silvany R, Dougherty J. 1990. In vivo and in vitro collagenolytic activity of Acanthamoeba castellanii. Investigative Ophthalmology and Visual Science, 31, 2235–2240. (In the text)
  38. Henrissat B, Callebaut I, Mornon JP, Fabrega S, Lehn P, Davies G. 1995. Conserved catalytic machinery and the prediction of a common fold for several families of glycosyl hydrolases. Proceedings of the National Academy of Science USA, 92(15), 7090–7094. [CrossRef] (In the text)
  39. Henrissat B, Davies G. 1995. Structures and mechanisms of glycosyl hydrolases. Structure, 3(9), 853–859. [CrossRef] [PubMed] (In the text)
  40. Hong YC, Lee WM, Kong HH, Jeong HJ, Chung DI. 2004. Molecular cloning and characterization of a cDNA encoding a laminin-binding protein (AhLBP) from Acanthamoeba healyi. Experimental Parasitology, 106, 95–102. [CrossRef] [PubMed] (In the text)
  41. Ikeda Y, Miyazaki D, Yakura K, Kawaguchi A, Ishikura R, Inoue Y, Mito T, Shiraishi A, Ohashi Y, Higaki S, Itahashi M, Fukuda M, Shimomura Y, Yagita K. 2012. Assessment of real-time polymerase chain reaction detection of Acanthamoeba and prognosis determinants of Acanthamoeba keratitis. Ophthalmology, 119, 1111–1119. [CrossRef] [PubMed] (In the text)
  42. Im K. 1990. Pathogenic free-living amoebae. Korean Journal of Parasitology, 28, 29–39. [CrossRef] (In the text)
  43. Kao PM, Tung MC, Hsu BM, Tsai HL, She CY, Shen SM, Huang WC. 2013. Real-time PCR method for the detection and quantification of Acanthamoeba species in various types of water samples. Parasitology Research, 112(3), 1131–1136. [CrossRef] [PubMed] (In the text)
  44. Kandori M, Inoue T, Shimabukuro M, Hayashi H, Hori Y, Maeda N, Tano Y. 2010. Four cases of Acanthamoeba keratitis treated with phototherapeutic keratectomy. Cornea, 29(10), 1199–1202. [CrossRef] [PubMed] (In the text)
  45. Kashiwabuchi RT, Carvalho FR, Khan YA, de Freitas D, Foronda AS, Hirai FE, Campos MS, McDonnell PJ. 2011. Assessing efficacy of combined riboflavin and UV-A light (365 nm) treatment of Acanthamoeba trophozoites. Investigative Ophthalmology and Visual Science, 52(13), 9333–9338. [CrossRef] (In the text)
  46. Khan NA. 2009. Acanthamoeba – Biology and Pathogenesis. Caister Academic Press: Norfolk, Great Britain, 290 p. (In the text)
  47. Khan NA. 2006. Acanthamoeba: biology and increasing importance in human health. FEMS Microbiology Reviews, 30, 564–595. [CrossRef] [PubMed] (In the text)
  48. Khan NA. 2001. Pathogenicity, morphology and differentiation of Acanthamoeba. Current Microbiology, 43, 391–395. [CrossRef] [PubMed] (In the text)
  49. Khan YA, Kashiwabuchi RT, Martins SA, Castro-Combs JM, Kalyani S, Stanley P, Flikier D, Behrens A. 2011. Riboflavin and ultraviolet light a therapy as an adjuvant treatment for medically refractive Acanthamoeba keratitis: report of 3 cases. Ophthalmology, 118(2), 324–331. [CrossRef] [PubMed] (In the text)
  50. Kim JY, Na BK, Song KJ, Park MH, Park YK, Kim TS. 2012. Functional expression and characterization of an iron-containing superoxide dismutase of Acanthamoeba castellanii. Parasitology Research, 111, 1673–1682. [CrossRef] [PubMed] (In the text)
  51. Kitzmann AS, Goins KM, Sutphin JE, Wagoner MD. 2009. Keratoplasty for treatment of Acanthamoeba keratitis. Ophthalmology, 116, 864–869. [CrossRef] [PubMed] (In the text)
  52. Lim N, Goh D, Bunce C, Xing W, Fraenkel G, Poole TR, Ficker L. 2008. Comparison of polyhexamethylene biguanide and chlorhexidine as monotherapy agents in the treatment of Acanthamoeba keratitis. American Journal of Ophthalmology, 145, 130–135. [CrossRef] [PubMed] (In the text)
  53. Lorenzo-Morales J, Kliescikova J, Martínez-Carretero E, De Pablos LM, Profotova B, Nohynkova E, Osuna A, Valladares B. 2008. Glycogen phosphorylase in Acanthamoeba spp.: determining the role of the enzyme during the encystment process using RNA interference. Eukaryotic Cell, 7(3), 509–517. [CrossRef] [PubMed] (In the text)
  54. Lorenzo-Morales J, Martín-Navarro CM, López-Arencibia A, Arnalich-Montiel F, Piñero JE, Valladares B. 2013. Acanthamoeba keratitis: an emerging disease gathering importance worldwide? Trends in Parasitology, 29(4), 181–187. [CrossRef] [PubMed] (In the text)
  55. Lorenzo-Morales J, Ortega-Rivas A, Foronda P, Abreu-Acosta N, Ballart D, Martínez E, Valladares B. 2005. RNA interference (RNAi) for the silencing of extracellular serine proteases genes in Acanthamoeba: Molecular analysis and effect on pathogenecity. Molecular and Biochemical Parasitology, 144, 10–15. [CrossRef] [PubMed] (In the text)
  56. Marciano-Cabral F, Cabral G. 2003. Acanthamoeba spp. as agents of disease in humans. Clinical Microbiology Reviews, 16(2), 273–307. [CrossRef] [PubMed] (In the text)
  57. Martín-Navarro CM, Lorenzo-Morales J, López-Arencibia A, Reyes-Batlle M, Piñero JE, Valladares B, Maciver SK. 2014. Evaluation of Acanthamoeba myosin-IC as a potential therapeutic target. Antimicrobial Agents and Chemotherapy, 58(4), 2150–2155. [CrossRef] [PubMed] (In the text)
  58. Martín-Navarro CM, Lorenzo-Morales J, Machin RP, López-Arencibia A, García-Castellano JM, de Fuentes I, Loftus B, Maciver SK, Valladares B, Piñero JE. 2013. Inhibition of HMG-CoA reductase and the application of statins as a novel effective therapeutic approach against Acanthamoeba infections. Antimicrobial Agents and Chemotherapy, 57(1), 375–381. [CrossRef] [PubMed] (In the text)
  59. Mathers WD, Nelson SE, Lane JL, Wilson ME, Allen RC, Folberg R. 2000. Confirmation of confocal microscopy diagnosis of Acanthamoeba keratitis using polymerase chain reaction analysis. Archives of Ophthalmology, 118, 178–183. [CrossRef] [PubMed] (In the text)
  60. Mattana A, Cappai V, Alberti L, Serra C, Fiori PL, Cappuccinelli P. 2002. ADP and other metabolites released from Acanthamoeba castellanii lead to human monocytic cell death through apoptosis and stimulate the secretion of proinflammatory cytokines. Infection and Immunity, 70, 4424–4432. [CrossRef] [PubMed] (In the text)
  61. Maubon D, Dubosson M, Chiquet C, Yera H, Brenier-Pinchart MP, Cornet M, Savy O, Renard E, Pelloux H. 2012. A one-step multiplex PCR for Acanthamoeba keratitis diagnosis and quality samples control. Investigative Ophthalmology and Visual Science, 53(6), 2866–2872. [CrossRef] (In the text)
  62. Mazur T, Hadas E, Iwanicka I. 1995. The duration of the cyst stage and the viability and virulence of Acanthamoeba isolates. Tropical Medicine and Parasitology, 46, 106–108. (In the text)
  63. McClellan K, Howard K, Niederkorn JY, Alizadeh H. 2001. Effect of steroids on Acanthamoeba cysts and trophozoites. Investigative Ophthalmology and Visual Science, 42, 2885–2893. (In the text)
  64. Michalek M, Sönnichsen FD, Wechselberger R, Dingley AJ, Hung CW, Kopp A, Wienk H, Simanski M, Herbst R, Lorenzen I, Marciano-Cabral F, Gelhaus C, Gutsmann T, Tholey A, Grötzinger J, Leippe M. 2013. Structure and function of a unique pore-forming protein from a pathogenic Acanthamoeba. Nature Chemical Biology, 9, 37–42. [CrossRef] [PubMed] (In the text)
  65. Moon EK, Hong Y, Chung DI, Goo YK, Kong HH. 2014. Down-regulation of cellulose synthase inhibits the formation of endocysts in Acanthamoeba. Korean Journal of Parasitology, 52(2), 131–135. [CrossRef] (In the text)
  66. Mortazavi PN, Keisary E, Loh LN, Jung SY, Khan NA. 2011. Possible roles of phospholipase A2 in the biological activities of Acanthamoeba castellanii (T4 genotype). Protist, 162, 168–176. [CrossRef] [PubMed] (In the text)
  67. Na BK, Cho JH, Song CY, Kim TS. 2002. Degradation of immunoglobulins, protease inhibitors and interleukin-1 by a secretory proteinase of Acanthamoeba castellanii. Korean Journal of Parasitology, 40, 93–99. [CrossRef] (In the text)
  68. Na BK, Kim JC, Song CY. 2001. Characterization and pathogenetic role of proteinase from Acanthamoeba castellanii. Microbial Pathogenesis, 30, 39–48. [CrossRef] [PubMed] (In the text)
  69. Nguyen TH, Weisenthal RW, Florakis GJ, Reidy JJ, Gaster RN, Tom D. 2010. Penetrating keratoplasty in active Acanthamoeba keratitis. Cornea, 29, 1000–1004. [CrossRef] [PubMed] (In the text)
  70. Niederkorn JY, Alizadeh H, Leher H, McCulley JP. 1999. The pathogenesis of Acanthamoeba keratitis. Microbes and Infection, 1, 437–443. [CrossRef] (In the text)
  71. Page FC, Siemensma FJ. 1991. Nackte Rhizopoda und Heliozoea, in Protozoenfauna, Band 2, Matthes D (Hrsg.). G. Fischer: Stuttgart. (In the text)
  72. Parthasarathy A, Tan DT. 2007. Deep lamellar keratoplasty for Acanthamoeba keratitis. Cornea, 26(8), 1021–1023. [CrossRef] [PubMed] (In the text)
  73. Pellegrin JL, Ortega-Barria E, Barza M, Baum J, Pereira ME. 1991. Neuraminidase activity in Acanthamoeba species trophozoites and cysts. Investigative Ophthalmology and Visual Science, 32, 3061–3066. (In the text)
  74. Pellegrin JL, Ortega-Barria E, Prioli RP, Meijia JS, Pereira ME. 1992. The neuraminidases of Trypanosoma cruzi and Acanthamoeba castellanii are immunologically related. Tropical Medicine and Parasitology, 43, 33–37. (In the text)
  75. Pérez-Serrano J, Martínez J, Pérez B, Bernadina WE, Rodríguez-Caabeiro F. 2000. In vitro shock response to different stressors in free living and pathogenic Acanthamoeba. International Journal of Parasitology, 30(7), 829–835. [CrossRef] (In the text)
  76. Pettit DA, Williamson J, Cabral GA, Marciano-Cabral F. 1996. In vitro destruction of nerve cell cultures by Acanthamoeba spp.: a transmission and scanning electron microscopy study. Journal of Parasitology, 82, 769–777. [CrossRef] (In the text)
  77. Podlipaeva IuI, Shmakov LA, Gilichinskiĭ DA, Gudkov AV. 2006. Heat shock protein of HSP70 family revealed in some contemporary freshwater Amoebae and in Acanthamoeba sp. from cysts isolated from permafrost samples. Tsitologiia, 48(8), 691–694. (In the text)
  78. Polat ZA, Obwaller A, Vural A, Walochnik J. 2012. Efficacy of miltefosine for topical treatment of Acanthamoeba keratitis in Syrian hamsters. Parasitology Research, 110(2), 515–522. [CrossRef] [PubMed] (In the text)
  79. Polat ZA, Walochnik J, Obwaller A, Vural A, Dursun A, Arici MK. 2014. Miltefosine and polyhexamethylene biguanide: a new drug combination for the treatment of Acanthamoeba keratitis. Clinical and Experimental Ophthalmology, 42(2), 151–158. [CrossRef] (In the text)
  80. Pussard M, Pons R. 1977. Morphologie de la paroi kystique et taxonomie du genre Acanthamoeba (Protozoa, Amoebida). Protistologica, 8, 557–598. (In the text)
  81. Qvarnstrom Y, Visvesvara GS, Sriram R, da Silva AJ. 2006. Multiplex real-time PCR assay for simultaneous detection of Acanthamoeba spp., Balamuthia mandrillaris, and Naegleria fowleri. Journal of Clinical Microbiology, 44(10), 3589–3595. [CrossRef] [PubMed] (In the text)
  82. Ren M, Gao L, Wu X. 2010. TLR4: the receptor bridging Acanthamoeba challenge and intracellular inflammatory responses in human corneal cell lines. Immunology and Cell Biology, 88, 529–536. [CrossRef] [PubMed] (In the text)
  83. Ren MY, Wu XY. 2011. Toll-like receptor 4 signalling pathway activation in a rat model of Acanthamoeba keratitis. Parasite Immunology, 33, 25–33. [CrossRef] [PubMed] (In the text)
  84. Rivière D, Szczebara FM, Berjeaud JM, Frère J, Héchard Y. 2006. Development of a real-time PCR assay for quantification of Acanthamoeba trophozoites and cysts. Journal of Microbiological Methods, 64(1), 78–83. [CrossRef] [PubMed] (In the text)
  85. Robaei D, Carnt N, Minassian DC, Dart JK. 2014. The impact of topical corticosteroid use before diagnosis on the outcome of Acanthamoeba keratitis. Ophthalmology, 121(7), 1383–1388. [CrossRef] [PubMed] (In the text)
  86. Roberts CW, Henriquez FL. 2010. Drug target identification, validation, characterisation and exploitation for treatment of Acanthamoeba (species) infections. Experimental Parasitology, 126, 91–96. [CrossRef] [PubMed] (In the text)
  87. Rocha-Azevedo BD, Jamerson M, Cabral GA, Silva-Filho FC, Marciano-Cabral F. 2009. Acanthamoeba interaction with extracellular matrix glycoproteins: biological and biochemical characterization and role in cytotoxicity and invasiveness. Journal of Eukaryotic Microbiology, 56, 270–278. [CrossRef] (In the text)
  88. Rondinone CM. 2006. Therapeutic potential of RNAi in metabolic diseases. Biotechniques, 40, 31–36. [CrossRef] (In the text)
  89. Saheb E, Trzyna W, Bush J. 2013. An Acanthamoeba castellanii metacaspase associates with the contractile vacuole and functions in osmoregulation. Experimental Parasitology, 133, 314–326. [CrossRef] [PubMed] (In the text)
  90. Schroeder JM, Booton GC, Hay J, Niszl IA, Seal DV, Markus MB, Fuerst PA, Byers TJ. 2001. Use of subgenic 18S ribosomal DNA PCR and sequencing for genus and genotype identification of Acanthamoeba from humans with keratitis and from sewage sludge. Journal of Clinical Microbiology, 39, 1903–1911. [CrossRef] [PubMed] (In the text)
  91. Schuster FL. 2002. Cultivation of pathogenic and opportunistic free-living amebas. Clinical Microbiology Reviews, 15(3), 342–354. [CrossRef] [PubMed] (In the text)
  92. Schuster FL, Levandowsky M. 1996. Chemosensory responses of Acanthamoeba castellanii: visual analysis of random movement and responses to chemical signals. Journal of Eukaryotic Microbiology, 43, 150–158. [CrossRef] (In the text)
  93. Siddiqui R, Iqbal J, Maugueret MJ, Khan NA. 2012. The role of Src kinase in the biology and pathogenesis of Acanthamoeba castellanii. Parasites and Vectors, 5, 112. [CrossRef] (In the text)
  94. Sissons J, Alsam S, Jayasekera S, Khan NA. 2004. Ecto-ATPases of clinical and non-clinical isolates of Acanthamoeba. Microbial Pathogenesis, 37, 231–239. [CrossRef] [PubMed] (In the text)
  95. Sissons J, Alsam S, Jayasekera S, Kim KS, Stins M, Khan NA. 2004. Acanthamoeba induces cell-cycle arrest in the host cells. Journal of Medical Microbiology, 53, 711–717. [CrossRef] [PubMed] (In the text)
  96. Sissons J, Kim KS, Stins M, Jayasekera S, Alsam S, Khan NA. 2005. Acanthamoeba castellanii induces host cell death via a phosphatidylinositol 3-kinase-dependent mechanism. Infection and. Immunity, 73, 2704–2708. [CrossRef] [PubMed] (In the text)
  97. Stothard DR, Schroeder-Diedrich JM, Awwad MH, Gast RJ, Ledee DR, Rodriguez-Zaragoza S, Dean CL, Fuerst PA, Byers TJ. 1998. The evolutionary history of the genus Acanthamoeba and the identification of eight new 18S rDNA gene sequence types. Journal of Eukaryotic Microbiology, 45, 45–54. [CrossRef] (In the text)
  98. Sun X, Zhang Y, Li R, Wang Z, Luo S, Gao M, Deng S, Chen W, Jin X. 2006. Acanthamoeba keratitis: clinical characteristics and management. Ophthalmology, 113, 412–416. [CrossRef] [PubMed] (In the text)
  99. Szentmáry N, Goebels S, Matoula P, Schirra F, Seitz B. 2012. Die Akanthamöbenkeratitis – ein seltenes und oft spät diagnostiziziertes Chamäleon. Klinische Monatsblätter für Augenheilkunde, 229(5), 521–528. [CrossRef] (In the text)
  100. Taylor WM, Pidherney MS, Alizadeh H, Niederkorn JY. 1995. In vitro characterization of Acanthamoeba castellanii cytopathic effect. Journal of Parasitology, 81, 603–609. [CrossRef] (In the text)
  101. Thomas PA, Kuriakose T. 1990. Rapid detection of Acanthamoeba cysts in corneal scrapings by lactophenol cotton blue staining. Archives of Ophthalmology, 108(2), 168. [CrossRef] [PubMed] (In the text)
  102. Tripathi T, Abdi M, Alizadeh H. 2013. Role of phospholipase A2 (PLA2) inhibitors in attenuating apoptosis of the corneal epithelial cells and mitigation of Acanthamoeba keratitis. Experimental Eye Research, 113, 182–191. [CrossRef] [PubMed] (In the text)
  103. Trzyna WC, Legras XD, Cordingley JS. 2008. A type-1 metacaspase from Acanthamoeba castellanii. Microbiology Research, 163, 414–423. [CrossRef] (In the text)
  104. Tu EY, Joslin CE, Sugar J, Shoff ME, Booton GC. 2008. Prognostic factors affecting visual outcome in Acanthamoeba keratitis. Ophthalmology, 115, 1998–2003. [CrossRef] [PubMed] (In the text)
  105. Tu EY, Joslin CE, Nijm LM, Feder RS, Jain S, Shoff ME. 2009. Polymicrobial keratitis: Acanthamoeba and infectious crystalline keratopathy. American Journal of Ophthalmology, 148, 13–19. [CrossRef] [PubMed]
  106. Turner NA, Russell AD, Furr JR, Lloyd D. 2004. Resistance, biguanide sorption and biguanide-induced pentose leakage during encystment of Acanthamoeba castellanii. Journal of Applied Microbiology, 96(6), 1287–1295. [CrossRef] [PubMed] (In the text)
  107. Turner NA, Russell AD, Furr JR, Lloyd D. 2000. Emergence of resistance to biocides during differentiation of Acanthamoeba castellanii. Journal of Antimicrobials and Chemotherapy, 46(1), 27–34. [CrossRef] (In the text)
  108. Ueki N, Eguchi H, Oogi Y, Shiota H, Yamane S, Umazume H, Mizui K. 2009. Three cases of Acanthamoeba keratitis diagnosed and treated in the early stage. Journal of Medical Investigation, 56(3–4), 166–169. [CrossRef] (In the text)
  109. Van Klink F, Alizadeh H, Stewart GL, Pidherney MS, Silvany RE, He Y, McCulley JP, Niederkorn JY. 1992. Characterization and pathogenic potential of a soil isolate and an ocular isolate of Acanthamoeba castellanii in relation to Acanthamoeba keratitis. Current Eye Research, 11, 1207–2012. [CrossRef] [PubMed] (In the text)
  110. Villani E, Baudouin C, Efron N, Hamrah P, Kojima T, Patel SV, Pflugfelder SC, Zhivov A, Dogru M. 2014. In vivo confocal microscopy of the ocular surface: from bench to bedside. Current Eye Research, 39(3), 213–231. [CrossRef] [PubMed] (In the text)
  111. Visvesvara GS, Moura H, Schuster FL. 2007. Pathogenic and opportunistic free-living amoebae: Acanthamoeba spp., Balamuthia mandrillaris, Naegleria fowleri, and Sappinia diploidea. FEMS Immunology and Medical Microbiology, 50(1), 1–26. [CrossRef] [PubMed] (In the text)
  112. Visvesvara GS. 2010. Amebic meningoencephalitides and keratitis: challenges in diagnosis and treatment. Current Opinion in Infectious Diseases, 23(6), 590–594. [CrossRef] [PubMed] (In the text)
  113. Walochnik J, Michel R, Aspöck H. 2004. A molecular biological approach to the phylogenetic position of the genus Hyperamoeba. Journal of Eukaryotic Microbiology, 51(4), 433–440. [CrossRef] (In the text)
  114. Walochnik J, Obwaller A, Aspöck H. 2000. Correlations between morphological, molecular biological, and physiological characteristics in clinical and nonclinical isolates of Acanthamoeba spp. Applied and Environmental Microbiology, 66(10), 4408–4413. [CrossRef] [PubMed] (In the text)
  115. Walochnik J, Obwaller A, Haller-Schober EM, Aspöck H. 2001. Anti-Acanthamoeba IgG, IgM, and IgA immunoreactivities in correlation to strain pathogenicity. Parasitology Research, 87(8), 651–656. [CrossRef] [PubMed] (In the text)
  116. Walochnik J, Scheikl U, Haller-Schober EM. 2014. Twenty years of Acanthamoeba diagnostics in Austria. Journal of Eukaryotic Microbiology, 2014 July 22. doi: 10.1111/jeu.12149. [Epub ahead of print]. (In the text)
  117. Wynter-Allison Z, Lorenzo Morales J, Calder D, Radlein K, Ortega-Rivas A, Lindo JF. 2005. Acanthamoeba infection as a cause of severe keratitis in a soft contact lens wearer in Jamaica. American Journal of Tropical Medicine and Hygiene, 73(1), 92–94. (In the text)
  118. Zegans ME, Becker HI, Budzik J, O’Toole G. 2002. The role of bacterial biofilms in ocular infections. DNA and Cell Biology, 21, 415–420. [CrossRef] [PubMed] (In the text)

Cite this article as: Lorenzo-Morales J, Khan NA & Walochnik J: An update on Acanthamoeba keratitis: diagnosis, pathogenesis and treatment. Parasite, 2015, 22, 10

All Tables

Table 1.

Important characteristics for the differential diagnosis of Acanthamoeba keratitis (AK) compared to keratitis due to other infectious agents.

Table 2.

Neff’s Amoeba Saline (AS) [71]. 10 mL of each stock solution (10×) are added to 950 mL dH2O, mixed, sterilized by filtration and aliquoted into needed volumes.

Table 3.

PYG medium [71]. Compounds are weighted into a 1 L bottle, filled up to 1 L with dH2O, mixed and sterilized by filtration.

All Figures

thumbnail Figure 1.

(A) Corneal melting and vascularization in a patient with Acanthamoeba keratitis. (B) Observed corneal damage in AK is shown after sodium fluorescein application. Original.

In the text
thumbnail Figure 2.

Overview of the diagnostic procedure for Acanthamoeba keratitis.

In the text
thumbnail Figure 3.

Acanthamoeba trophozoites with the characteristic acanthopodia (A) in phase contrast, (B) in bright field microscopy. Scale bar: 10 μm. Originals.

In the text
thumbnail Figure 4.

Acanthamoeba cysts in interference contrast microscopy (A) morphological group I, (B) morphological group II, (C) morphological group III. Scale bar: 10 μm. Original.

In the text
thumbnail Figure 5.

Acanthamoeba trophozoites observed in culture in a case of severe AK infection.

In the text
thumbnail Figure 6.

Factors contributing to the pathogenicity of Acanthamoeba.

In the text
thumbnail Figure 7.

Schematics of Acanthamoeba-mediated corneal damage. “Blast” refers to damage.

In the text
thumbnail Figure 8.

Acanthamoeba-mediated corneal epithelial cell death.

In the text