The global challenge of Candida auris in the intensive care unit

Following the first isolation in Japan, cases have been reported in several countries in five continents. Although uncommon for fungi, C. auris has the ability to cause outbreaks, as seen in India, the UK, Spain, the USA, Venezuela, Colombia, and South Africa [1]. It is still debated whether C. auris emerged in one region with subsequent spreading to others, or if it emerged independently across different countries. Evidence from genomic sequencing demonstrates different clades of C. auris show strong geographic structure, with independent emergence in East and South Asia, Africa, and South America [1, 5, 6].

To date, there are not established minimum inhibitory concentrations (MICs) breakpoints for susceptibility testing of C. auris. Antifungal susceptibility data from three continents demonstrated that nearly 40% were MDR, with strains being resistant to fluconazole (90%), amphotericin B (30–40%) and echinocandins (5–10%). Moreover, a small percentage were also resistant to all antifungals actually available [4, 6]. C. auris demonstrates a high propensity to develop antifungal resistance under selective pressure. Recent studies demonstrated mutations in ERG11 (encoding lanosterol demethylase, the target of azoles) and FKS1 genes (encoding 1,3-beta-glucan synthase, the target of echinocandins) [1, 7].

The recommended antifungals for C. auris treatment are mainly based on in vitro testing and on the most frequently retrieved resistance profiles. Echinocandins are the recommended first-line treatment, pending specific susceptibility testing. Lipid formulation of amphotericin B should be an alternative in patients not responding to echinocandins. Close monitoring to early detect therapeutic failures and evolution of antifungal resistance is needed. New antifungals (e.g., SCY-078, APX001A/APX001, and rezafungin) have been tested with success but they are not available to date for clinical use [1].

Unlike others Candida species, C. auris can colonize different anatomical sites (e.g., skin, skin, rectum, axilla, stool) and contaminate hospital equipment and surfaces, creating a vicious cycle of acquisition, spreading, and infection, particularly in ICUs. Indeed, bed, chairs, and monitoring tools (e.g., pulse oximeters, temperature probes) were contaminated during outbreaks [8]. Recently, Eyre et al. [9] published the results of a patients’ and hospital environmental screening program in Oxford, UK, after 70 patients (66 admitted to a neuro-ICU) were identified as being colonized or infected by C. auris. Seven patients developed an invasive infection during hospital stay. C. auris was detected mainly on skin-surface axillary temperature probes and other reusable tools. In patients monitored with skin-surface temperature probes, the risk of C. auris infection/colonization was seven times higher. Adoption of specific bundles of infection control had no significant effects until removal of the temperature probes [9].

Recent studies have confirmed that C. auris can form biofilms, with a high variation of capacity of production depending on the C. auris strain considered [10]. Biofilm may present reduced susceptibility to hydrogen peroxide and chlorhexidine [11].

Quaternary ammonium compounds and cationic surface-active products seem to be ineffective against C. auris. Chlorine-based products appear to be the most effective for environmental surface disinfection [12]. Chlorine-based disinfectants (at a concentration of 1000 ppm), hydrogen- peroxide, or other disinfectants with documented fungicidal activity are recommended for environmental cleaning by the European CDC (ECDC) [13].

CDC and ECDC released recommendations for C. auris case and outbreak management [13]. Usually, outbreaks follow an exponential increase in the number of affected patients. It is mandatory to trace contacts with the aim to achieve early identification and screening of possible colonized patients that might be responsible for persistence of C. auris. Patients potentially or already colonized should be placed in single rooms with contact isolation precautions. Screening should be applied for contacts and patients previously hospitalized in healthcare settings where C. auris isolation was confirmed. Hand hygiene (with alcohol or chlorhexidine hand rubs), wearing of protective clothing, and skin and environmental/equipment decontamination should be performed to prevent ongoing transmission.

Aiming to support implementation measures on global surveillance on antimicrobial resistances, in 2016, the World Health Organization [14] launched the Global Resistance Surveillance System (GLASS). The emergence of C. auris and progressive spread of infections caused by other resistant pathogens has strengthened the need for a surveillance network for antimicrobial resistance globally for critically ill patients’ safety.

It is hard to predict future C. auris diffusion. There will be outbreaks also in countries in which C. auris has been not reported yet? Will new MDR clones continue to emerge? Will we be able to apply effective antifungal stewardship programs and control measures? By now, global surveillance, improving knowledge, and taking care of the A.U.R.I.S. major issues may be the best ways to face C. auris challenge.