Since the 1960s, methicillin-resistant Staphylococcus aureus (MRSA) has emerged, disseminated globally and become a leading cause of bacterial infections in both health-care and community settings. However, there is marked geographical variation in MRSA burden owing to several factors, including differences in local infection control practices and pathogen-specific characteristics of the circulating clones. Different MRSA clones have resulted from the independent acquisition of staphylococcal cassette chromosome mec (SCCmec), which contains genes encoding proteins that render the bacterium resistant to most β-lactam antibiotics (such as methicillin), by several S. aureus clones. The success of MRSA is a consequence of the extensive arsenal of virulence factors produced by S. aureus combined with β-lactam resistance and, for most clones, resistance to other antibiotic classes. Clinical manifestations of MRSA range from asymptomatic colonization of the nasal mucosa to mild skin and soft tissue infections to fulminant invasive disease with high mortality. Although treatment options for MRSA are limited, several new antimicrobials are under development. An understanding of colonization dynamics, routes of transmission, risk factors for progression to infection and conditions that promote the emergence of resistance will enable optimization of strategies to effectively control MRSA. Vaccine candidates are also under development and could become an effective prevention measure.
Staphylococcus aureus is a Gram-positive, nonmotile, coagulase-positive coccoid bacterium of the Firmicutes phylum. Although the Staphylococcus genus includes 52 species and 28 subspecies (List of Prokaryotic names with Standing in Nomenclature), S. aureus is by far the most clinically relevant. S. aureus is found in the human commensal microbiota of the nasal mucosa in 20–40% of the general population1,2. The reported prevalence varies owing to differences in the size and demographics of the study populations, quality of sampling and culture techniques utilized3. When the cutaneous and mucosal barriers are disrupted, for example, owing to chronic skin conditions, wounds or surgical intervention, S. aureus can gain access to the underlying tissues or the bloodstream and cause infection. Persons with invasive medical devices (such as peripheral and central venous catheters) or compromised immune systems are particularly vulnerable to S. aureus infection4.
Methicillin-resistant S. aureus (MRSA) was first described in England in 1961 (Ref.5), soon after methicillin was introduced into clinical practice. Methicillin was initially widely used; however, because of its toxicity, it is now no longer marketed for human use and has largely been replaced by similar, more-stable penicillins such as oxacillin, flucloxacillin and dicloxacillin6. Nevertheless, the term methicillin-resistant S. aureus continues to be used. In the decade following its initial description, MRSA was responsible for hospital outbreaks (health-care-associated MRSA (HA-MRSA)) in many parts of the world7. A substantial change in MRSA epidemiology was observed when it was detected in individuals without previous health-care contact (referred to as community-associated MRSA (CA-MRSA)), notably among indigenous populations in Australia in the 1980s8 and otherwise healthy persons, including children, in the United States in the 1990s9. Since the mid-2000s, it has also been associated with livestock exposure (livestock-associated MRSA (LA-MRSA))10.
Several S. aureus clones (that is, bacteria that are indistinguishable from each other by a variety of genetic tests (for example, pulsed-field gel electrophoresis, multilocus enzyme electrophoresis or ribotyping) or that are so similar that they are presumed to be derived from a common parent11) have developed into MRSA by uptake via horizontal gene transfer of staphylococcal cassette chromosome mec (SCCmec)12, a mobile genetic element that encodes the genes mecA or mecC, which confer resistance to methicillin and, therefore, to most β-lactam antibiotics. MRSA is often also resistant to multiple other antibiotic classes. Indeed, S. aureus has the remarkable ability to acquire resistance to any antibiotic7, which has major implications for current as well as future treatment options for this pathogen.
Individuals with MRSA colonization or carriage (that is, the presence of bacteria that do not cause a detectable host immune response, cellular damage or clinical signs and symptoms of infection) have an increased risk of subsequent infection and are an important source of person-to-person transmission. Health-care facilities host persons who are predisposed to infection (for example, owing to invasive procedures and/or immune compromise) and are environments with high antibiotic selection pressure (which can contribute to the selection of antimicrobial resistance in bacteria) and frequent contact between individuals. These conditions have facilitated the epidemic spread of MRSA in hospitals; MRSA is now endemic in many health-care facilities throughout the world and, as a consequence, it has become a major focus for infection control efforts globally.
This Primer reviews the epidemiology, pathophysiology, diagnosis, prevention, management and clinical effect of MRSA, focusing on HA-MRSA, and discusses future research priorities. In some aspects of the epidemiology and pathophysiology, where methicillin resistance does not substantially affect the behaviour of the species, data regarding S. aureus in general have also been included.
The emergence and worldwide spread of MRSA represent some of the most important events in the epidemiology of infectious diseases. Although MRSA was first reported in the early 1960s5, whole-genome sequencing (WGS) of 209 early MRSA isolates suggests that MRSA emerged in the mid-1940s — that is, much earlier than the introduction of methicillin13. In fact, it has been hypothesized that it was the extensive use of penicillin rather than the introduction of methicillin that drove the emergence of MRSA13.
Many countries have experienced an increasing burden of MRSA since the 1960s. The burden of MRSA has notable geographical variation, ranging from low prevalence in Scandinavia to the highest prevalence in parts of America and Asia14 (Fig. 1). The spread of MRSA seems to occur by at least two mechanisms: spread of existing resistant clones and acquisition of SCCmec by a methicillin-sensitive S. aureus (MSSA) strain (a strain is a descriptive subdivision of a species based on phenotypic and/or genotypic characteristics11). Details of the mechanism of horizontal transfer of SCCmec are not well understood, but epidemiological evidence shows that this resistance mechanism has spread to most clones of S. aureus, in both human and animal pathogenic strains15,16. The following sections discuss the epidemiology of MRSA in different regions; in general, less comprehensive data are available from low-income and middle-income countries.
MRSA in Europe
Surveillance data from European countries show a general trend towards increasing MRSA prevalence from the north to the south of the continent, with <5% of S. aureus isolated from invasive infections being methicillin-resistant in northern Europe (for example, the Netherlands, Norway, Sweden and Denmark) compared with 25–50% in southern Europe (for example, Portugal, Spain, Italy and Greece)17 (Fig. 2). Varying infection control practices and antimicrobial usage are thought to contribute to the observed differences18.
After years of increasing MRSA prevalence, since the early 2000s, steady or decreasing prevalence has been observed in a number of countries17 (Fig. 2). This decline has been associated with the implementation of improved national control interventions. However, some experts argue that widespread declines in previously hyperendemic MRSA clones are attributable to changes in the organism itself, with loss in survival fitness resulting in shifts in circulating clones19,20.
With the declines largely occurring in HA-MRSA, there has been increasing recognition of animal reservoirs for human MRSA in Europe, particularly from food-producing animals such as pigs, cattle and poultry21. This LA-MRSA, predominantly belonging to clonal complex 398 (CC398), has primarily caused infections in those who work with livestock (particularly in the Netherlands, northwestern Germany22 and Spain23), but LA-MRSA infections have also been observed among the general population24,25. However, at present, sustained person-to-person transmission of LA-MRSA seems to be uncommon25,26.
MRSA in America
In the United States, ∼53% of S. aureus clinical isolates were methicillin-resistant in 2005 (Ref.27). MRSA has also been identified as the most common cause of skin and soft tissue infections (SSTIs) presenting to US hospital emergency departments, which is largely attributed to the emergence of CA-MRSA (particularly the USA300 clone in the early 2000s)28,29 (Fig. 3). The changes in epidemiology since the emergence of CA-MRSA in the country have made the distinction between CA-MRSA and HA-MRSA less clear30,31. A parallel epidemic of CA-MRSA closely related to USA300, the USA300 Latin-American variant (USA300-LV), was first identified in Colombia in 2005 and has emerged as the most prevalent CA-MRSA clone in northern South America32. The geographical spread of USA300 clones from South America to Europe has also been documented by genomic analysis of MRSA isolates in Switzerland33.
Similar to experiences in Europe, the incidence of HA-MRSA in the United States has shown decreasing trends since 2005, with hospital-onset HA-MRSA infections decreasing by 54%34. In 2007, Veterans Affairs Hospitals throughout the United States introduced a multifaceted prevention strategy including universal MRSA screening, contact precautions, hand hygiene promotion and institutional culture change35. This programme was associated with a significant reduction in MRSA infections by 62% in intensive care units (ICUs) and 45% in other hospital wards. In addition, many US states mandated specific MRSA control measures, and in 2008, the Centers for Medicare and Medicaid Services introduced financial penalties to hospitals for preventable health-care-acquired infections, although a large evaluation of this intervention showed no evidence that it was associated with a reduction in health-care-associated infections36.
MRSA in the Asia–Pacific region
MRSA is endemic in most hospitals in Asia, and some Asian countries have among the highest MRSA prevalence in the world37. However, most available data are from high-income countries (for example, Japan, South Korea and Singapore), with limited information from other nations. Although there is country-to-country variability, MRSA accounts for up to 50% of S. aureus bloodstream infections in parts of Asia37. Japan and South Korea have particularly high MRSA prevalence — with >70% of clinical isolates in South Korea being MRSA on the basis of regional surveillance data from 2011 (Refs37,38). High methicillin resistance rates are thought to be related to widespread inappropriate antimicrobial use (for example, self-medication and over-the-counter use) as well as high population density facilitating rapid transmission of multidrug-resistant organisms37. Nevertheless, some countries in Asia (for example, Taiwan39) that experienced a peak in HA-MRSA prevalence in the late 1990s have shown declining prevalence since the early 2000s38.
In Australia, among health-care-associated S. aureus, MRSA has accounted for 20–33% of isolates since 2001 (Ref.40). Like Europe and the United States, Australia has implemented a range of local and national interventions that have been associated with a reduction in HA-MRSA bloodstream infections since 2002 (Ref.41). Since the earliest reports of CA-MRSA in remote indigenous populations in Western Australia in the late 1980s8, several distinct CA-MRSA clones circulating in the region have been identified, including virulent clones such as sequence type 93 (ST93; Queensland clone) and ST30 (Southwest Pacific clone)42.
MRSA in Africa
MRSA prevalence data from Africa are variable in coverage and quality. Published data are available for South Africa, Nigeria and countries from the Mediterranean basin, but there is a paucity of data from other nations43. Most data are also from single-centre studies, and information from broader surveillance systems is lacking. In addition, most studies have relied on phenotypic methods to identify MRSA, and these tests might be less reliable than genotypic methods depending on the choice of antibiotic used to detect MRSA43.
MRSA prevalence is estimated at <50% in most countries, with several countries reporting prevalence of <25%43. However, MRSA prevalence has been increasing since the early 2000s in reports from most countries, although it has started to decrease in South Africa (from 36% in 2006 (Ref.44) to 24% during 2007–2011 (Ref.45))43. Differences in the availability and use of antimicrobials, incidence of HIV infection (a risk factor for MRSA colonization46) and infection control practices could potentially account for some of the variation between countries.
Staphylococcus aureus colonization
S. aureus colonization precedes the development of infection in most cases47. Less commonly, infection can occur in the absence of known S. aureus colonization, for example, as a result of contamination of catheters or wounds owing to suboptimal infection control practices by health-care workers. The principal site of S. aureus colonization is the nose, although colonization at other sites occurs, notably in the throat and perineum48. Longitudinal studies have identified three temporal patterns of S. aureus (including both MSSA and MRSA) colonization49. Continuous S. aureus colonization was found in ∼15% of individuals (known as persistent carriers), intermittent colonization was present in 70% of individuals (which means that the majority of individuals can repeatedly acquire S. aureus and spontaneously clear it), and S. aureus was never detected in 15% of individuals (referred to as non-carriers)49. Similar results were found by other studies50. Studies exploring specific host polymorphisms in genes involved in the inflammatory response51 indicate that there are underlying host factors that determine the carriage status. However, the precise nature of these underlying factors is not completely understood. For MRSA in particular, the duration of colonization is variable, and reported estimates could be biased by antibiotic treatment, which can shorten the duration of colonization. In one study in patients with MRSA colonization at the time of hospital discharge52, the median duration of colonization was 282 days; in this population, 81% of individuals had chronic skin lesions, a known risk factor for MRSA colonization, which may have contributed to prolonged carriage. Besides host factors, factors associated with the pathogen itself as well as the nasal microbiota can influence host carrier status.
Dynamics of colonization. During S. aureus colonization, initial bacterial adherence to the host's epithelial cells is mediated by teichoic acid on the cell wall, whereas microbial surface components recognizing adhesive matrix molecules play a part at a later stage of nasal colonization53,54. Of these components, S. aureus clumping factor B (ClfB), has been studied in vitro and in human volunteers55. A wild-type strain and its single locus clfB knockout variant were inoculated into the nose; the knockout variant was cleared significantly more rapidly than the wild-type strain. However, ClfB-deficient strains can still interact with nasal cells, indicating that there are several independent microbial surface components that play a part in colonization56. It must also be noted that only one strain was used in this study.
Besides host and pathogen factors, the interaction of S. aureus with other nasal-colonizing species (for example, Corynebacterium spp., Propionibacterium acnes, Staphylococcus lugdunensis and Staphylococcus epidermidis) has a role in S. aureus colonization. Studies of the nasal microbiota have shown that the presence of some species correlates with the presence or absence of S. aureus (for example, S. epidermidis has been positively correlated with the presence of S. aureus)57,58. The organisms of the nasal microbiota are in competition with each other in several ways. For example, they compete for adhesion sites and nutrients: there are low amounts of nutrients in the human nose. S. aureus can survive in environments with lower levels of nutrients than coagulase-negative staphylococci can59, possibly owing to differences in metabolism, and hence is better adapted to the human nose. However, no difference in nutrient levels has been observed between carriers and non-carriers59. Microbiota species also compete by antibiosis, that is, certain strains can produce antimicrobial molecules that inhibit their microbial competitors. S. lugdunensis, for example, produces an antimicrobial compound called lugdunin that inhibits and destroys S. aureus (including MRSA) in vitro and in a mouse model, possibly by leading to rapid breakdown of bacterial energy resources60. In humans, nasal colonization with S. lugdunensis has been associated with a sixfold lower risk of colonization with S. aureus. These findings are certainly interesting but explain only a minority of carriage patterns, as S. lugdunensis colonization has been reported in only 9 – 26% of the general population60,61. Finally, S. aureus also competes by induction of host defences, that is, it induces the production of host antimicrobial proteins that are less harmful to S. aureus than to other commensal bacteria62. Many studies support the role of these mechanisms in the interactions between S. aureus and the commensal microbiota, but a single mechanism is insufficient to explain all observed carriage patterns.
S. aureus has an extensive arsenal of virulence factors (including adhesive, host-cell damaging and immunomodulatory molecules) that vary in their presence or specificity between clones63,64, a variability that is reflected by the high diversity of infections that S. aureus can cause65,66 (Table 1). Many virulence genes are found on mobile genetic elements; thus, their combination differs substantially between clones and even between closely related strains. The potential association of specific virulence factors with certain types or aggressiveness of S. aureus infections remains elusive, probably because many of these factors have redundant, partially overlapping functions. Furthermore, many virulence factors cannot be investigated in animal models because they are human-specific67. This section focuses on the most prominent virulence mechanisms and typical routes of invasion.
Initiation of infection. S. aureus SSTIs are usually initiated by bacterial transfer (probably via hand contact) from the major reservoir in the nose to open microlesions and wounds on the skin68,69 (Fig. 4a). S. aureus surface proteins (for example, fibronectin-binding protein A (FnBPA), FnBPB, clumping factor A (ClfA), ClfB and collagen adhesin (Cna)) bind to extracellular matrix proteins and enable the bacteria to attach to and multiply on wounded tissues70. The capacity of S. aureus to adhere to and form biofilms (that is, sticky agglomerations of microorganisms embedded in an extracellular matrix; biofilms facilitate resistance to mechanical interference, host defences and antibiotic treatment) on artificial plastic or metal surfaces renders S. aureus a frequent cause of catheter-associated or joint-replacement-associated infections or of ventilator-associated pneumonia71. The subsequent influx of polymorphonuclear leukocytes (PMNs) is manipulated by S. aureus72, which shapes local inflammation73.
Abscess formation. The S. aureus coagulase proteins cause the formation of a fibrin pseudo-capsule surrounding bacteria and infiltrated PMNs, thereby preventing further leukocyte influx74 (Fig. 4b). S. aureus can impede opsonization, for instance, by production of a polysaccharide microcapsule66 and inhibition of the complement cascade75. However, the microcapsule is absent from important MRSA clones such as USA300 (Ref.63). Bacteria that are phagocytosed by PMNs can survive not only by counteracting PMN killing mechanisms72,76,77 but also by gradually destroying them with the help of cytolytic toxins. For example, many CA-MRSA clones produce pore-forming peptide (phenol soluble modulins (PSMs)) and protein toxins (α-toxin (also known as α-haemolysin) and several bi-component leukocidins such as the Panton–Valentine leukocidin (PVL)), which are host species-specific and bind to host leukocyte membranes, leading to the formation of pores and causing lytic cell death7,78, thereby increasing bacterial virulence. The massive inflammation elicited by activated or necrotic PMNs is further increased by S. aureus superantigen toxins, which bind to the major histocompatibility complex (MHC) class II of antigen-presenting cells and activate a large percentage of T cells nonspecifically, causing systemic hyper-inflammation referred to as ‘cytokine storms’79.
Systemic infection. Abscesses might be disrupted at later stages, releasing pus and live bacteria either towards the skin surface to promote pathogen transmission or towards the bloodstream to cause bacteraemia (Fig. 4c). Endovascular S. aureus can adhere to endothelial surfaces and platelets80,81, and this adhesion can initiate endocarditis, promote the formation of metastatic abscesses or induce bacterial uptake into endothelial cells, where the bacteria are difficult to reach by antibiotics and host defence molecules82. The agglutinating activity of coagulases is thought to contribute to systemic blood coagulation, and massive release of microorganism-associated molecular pattern molecules along with superantigen toxin-induced cytokine storms leads to fulminant systemic inflammation, sepsis and multi-organ failure if the endovascular spread of the bacteria cannot be contained83.
Regulation and adaptation. Most of the S. aureus virulence factors are differentially regulated by the accessory gene regulator (Agr) quorum-sensing system and other regulatory networks84. Many CA-MRSA clones such as USA300 have very active Agr systems, which leads to abundant expression of toxins and corresponds to a high capacity to cause SSTIs and invasive infections even in healthy individuals85. By contrast, many HA-MRSA clones contain an additional SCCmec-encoded phenol-soluble modulin (PSM; PSMmec), whose mRNA dampens Agr expression86. Accordingly, Agr is not very active in many HA-MRSA clones, which produce lower amounts of toxins but higher levels of adhesins and often cause bacteraemia via infected catheters or implanted medical devices. High virulence seems to even be detrimental for S. aureus in bacteraemia, with many isolates from bloodstream infections found to bear Agr-inactivating point mutations87. Elucidating virulence mechanisms whose inhibition would render S. aureus most vulnerable will be crucial for the development of new preventive and therapeutic strategies against MRSA.
Mechanisms of methicillin resistance
A crucial event in the evolution of S. aureus was the independent acquisition of the SCCmec complex in the early 1960s by several multidrug-resistant strains (resistant to penicillin, streptomycin, tetracycline and erythromycin88), rendering S. aureus resistant to most members of the β-lactam family of antibiotics5 (Fig. 3). Twelve known SCCmec types (I–XII) have been identified and are classified according to the type of cassette chromosome recombinase (ccr) complex and the class of the mec complex (Table 2). Types I, II and III are large SCCmec elements harbouring genes that confer resistance to several antibiotic classes and are primarily found in HA-MRSA89. Smaller elements, such as types IV and V SCCmec, are found in CA-MRSA, such as USA300 and USA400, but also in some widespread HA-MRSA clones, such as ST22-MRSA-IV, ST45-MRSA-IV and ST5-MRSA-VI (Fig. 3; Table 2). However, over the years, the distinction between the two epidemiological groups (HA-MRSA and CA-MRSA) has become blurred90.
All SCCmec types contain mecA (with the exception of type XI, which contains the homologue mecC), which encodes penicillin-binding protein 2a (PBP2a)91, a peptidoglycan transpeptidase. PBP2a has extremely low affinity for most β-lactam antibiotics; in the presence of β-lactam antibiotics that inhibit the function of the four native S. aureus penicillin-binding proteins (PBP1, PBP2, PPB3 and PBP4), PBP2a can take over the transpeptidase function of peptidoglycan biosynthesis (Fig. 5). A variant of mecA, named mecC, was identified in several S. aureus clones from animal and human isolates92; mecC encodes PBP2aLGA, named after the MRSA strain LGA251 from which it was first isolated. The mechanism of the control of β-lactam resistance in strain LGA251 was compared with the resistance mechanism in MRSA strains that carry mecA93,94; in the LGA251 strain, the level of methicillin resistance depends on mecC and on genes in the genetic background of the strain. In 2018, plasmid-borne methicillin resistance based on mecB has been identified in S. aureus95, but the mechanism of resistance encoded by mecB is yet to be clarified.
The primary control of the expression of mecA depends on the regulators encoded by mecI, mecR1 and mecR2 (Refs96,97) and on the regulators of the expression of the genes blaZ, blaI and blaRI (Ref.98). In addition, a surprisingly large number of genes — auxiliary or fem genes — has a profound influence on the resistant phenotype99. Three lines of evidence show that the level of mecA transcription is not predictive of the degree of methicillin resistance. First, the stringent stress response (that is, the bacterial reaction to different stress conditions, such as amino acid, fatty acid and iron limitation and heat shock) induced by the antibiotic mupirocin triggers an increase in PBP2a activity without affecting mecA transcription100. Second, inactivation of vraS (a member of the two-component regulatory system involving sensor protein VraS and response regulator protein VraR (VraS–VraR) involved in the control of the cell wall peptidoglycan biosynthesis) induced mecA transcription but did not increase the level of PBP2a activity101. Third, the chaperone foldase protein PrsA alters the levels of properly folded PBP2a in the membrane and, therefore, methicillin resistance without affecting mecA transcription102. The crucial role of the stringent stress response in mecA expression has been demonstrated using different experimental approaches99,103. A new line of investigation is focusing on the discovery of inhibitors of the stringent stress response that act in combination with β-lactam antibiotics103.
Diagnosis, screening and prevention
MRSA can cause a wide range of infections, such as SSTIs, pneumonia, osteoarticular infections, toxic shock syndrome (a rare, potentially life-threatening complication of infection with certain types of bacteria, including S. aureus, caused by the release of bacterial toxins and presenting with clinical features that can include fever, rash and hypotension) and bacteraemia, which may be complicated by endocarditis or severe sepsis4. The clinical presentations and risk factors for infection vary between HA-MRSA, CA-MRSA and LA-MRSA strains.
HA-MRSA is a cause of bacteraemia, pneumonia and, less commonly, SSTIs (particularly related to invasive procedures, for example, at surgical wounds or vascular access sites) in hospitalized patients105. The organism is often associated with invasive devices, such as intravascular catheters, endotracheal tubes and urinary catheters, probably owing to its capacity to form and survive in biofilms71.
Individuals who have had lengthy hospitalization, ICU admission, residency in a nursing home, antibiotic exposure (particularly to cephalosporins and fluoroquinolones, leading to antibiotic selection pressure), surgery, haemodialysis, chronic wounds or indwelling invasive devices have an increased risk of infection with HA-MRSA106. In addition, asymptomatic colonization with MRSA is a risk factor for subsequent infection, as individuals with MRSA colonization on admission had a relative risk of infection of 13 (95% CI 2.7–64.0) compared with those with MSSA colonization or 9.5 (95% CI 3.6–25.0) compared with those without S. aureus colonization107.
The most common clinical presentation for CA-MRSA is SSTI, which is often associated with abscesses or pus formation and accounts for ∼90% of cases29. CA-MRSA can cause particularly virulent infections. Fulminant infections with CA-MRSA strains have been reported, such as necrotizing pneumonia and necrotizing fasciitis (a rapidly progressive infection of the fascia with secondary necrosis of the subcutaneous tissues)108,109. Possible explanations for the increased virulence observed with CA-MRSA strains are very active Agr systems and the production of PVL. However, the presence of PVL varies from strain to strain, suggesting that other virulence factors contribute7.
Individuals with CA-MRSA infection usually lack the traditional risk factors associated with HA-MRSA strains. Populations or settings in which outbreaks of CA-MRSA infection have been reported include sports teams, military personnel and prisons110,111. On the basis of these observations, close contact with MRSA carriers (as occurs in households or other communal living environments), shared equipment or personal items and skin trauma (including trauma caused by injecting drug use or body shaving) might be associated with an increased risk of CA-MRSA infection. However, the distinction between CA-MRSA and HA-MRSA is becoming increasingly blurred, with transmission of CA-MRSA strains now being observed in health-care settings in some countries with high CA-MRSA burden, such as Greece112.
LA-MRSA has been associated with localized infections, such as SSTIs (including abscesses and wound infections) and otitis, as well as severe and invasive infections, such as bacteraemia, pneumonia, osteoarticular infections and endocarditis22. LA-MRSA predominantly colonizes and infects individuals who have direct contact with livestock (including cattle, horses, chickens and turkeys but particularly pigs) and their household members through transmission within the household25. However, there are reports of LA-MRSA in individuals with no connection to livestock, and in these cases, spread via environmental contamination or, less commonly, food-borne transmission has been postulated25.
Microbiological specimens from which MRSA can be isolated can be broadly classified into clinical and screening samples. Clinical samples (for example, specimens of purulent discharge, deep tissues, sputum and blood) are collected from individuals with symptoms or signs to investigate for active infection, whereas screening samples (for example, nasal, perineal and throat swabs) are obtained to detect asymptomatic colonization. An array of phenotypic and non-phenotypic methods can be used to detect MRSA directly from clinical or screening samples or to identify MRSA from presumptive staphylococcal colonies isolated from clinical samples. Phenotypic methods are usually preferred for clinical diagnostics.
Phenotypic methods. Pure S. aureus cultures, obtained by plating clinical samples on relevant culture media, can be screened for methicillin resistance by the disk-diffusion method. This method involves applying a cefoxitin disk on Mueller-Hinton agar or supplementing Mueller-Hinton agar with 6 micrograms per millilitre oxacillin and 4% NaCl (Clinical and Laboratory Standards Institute (CLSI) recommendations)113.
Initially, oxacillin was utilized as the marker antibiotic to detect MRSA; however, CLSI now recommends cefoxitin, as it is a better inducer of mecA and mecC than oxacillin and results in a clear recognizable phenotype113. The disk-diffusion method requires strict adherence to temperature (35 °C) and time (reading after 24 hours) to prevent false negative results. This is because the mecA encoded PBP2a is less efficient at crosslinking the pentapeptide chains of the cell wall peptidoglycan during cell wall synthesis, resulting in slower growth of the resistant isolates. This phenomenon leads to a heteroresistant population, wherein cells exhibit different levels of resistance and some are phenotypically susceptible114. The above-mentioned susceptibility testing guidelines enable the slower growing MRSA subpopulation to reach detectable levels in a heteroresistant population. Rarely, MRSA may present with phenotypic sensitivity to cefoxitin (and oxacillin) and require an overnight exposure to low concentrations of cefoxitin to exhibit resistance115. In this case, the presence of inducible mecA should be considered. Methicillin resistance in S. aureus colonies and cultures can also be detected by means of an antigen–antibody-based latex agglutination test that detects PBP2a by using an anti-PBP2a antibody. Moreover, several automated instruments performing identification and antimicrobial susceptibility testing of staphylococci have shown high sensitivities and specificities for the MRSA strains tested (reviewed in Ref.116).
For direct phenotypic detection of MRSA from positive blood cultures, there is renewed interest in refining bacteriophage-based assays. The KeyPath MRSA/MSSA blood culture test (MicroPhage Inc, Longmont, Colorado, USA) is a US FDA-approved, non-genotypic, rapid test for the identification of S. aureus and the detection of methicillin resistance directly from positive blood cultures. The assay detects the amplification of S. aureus-specific bacteriophages in the presence of methicillin with a turnaround time of 5 hours. Multicentre evaluation of this assay on 1,116 blood cultures showed 91.8% sensitivity, 98.3% specificity, 96.3% positive predictive value and 96.1% negative predictive value, with a median turnaround time of 16.9 hours versus 46.9 hours calculated for conventional tests for the identification of S. aureus and differentiating between MRSA and MSSA in positive blood cultures117.
Non-phenotypic methods. One of the most promising non-genotypic techniques for direct identification of pathogens from positive blood cultures is matrix-assisted laser desorption-ionization time-of-flight mass spectrometry (MALDI-TOF MS)118. Identification is based on the comparison of the protein profile obtained by mass spectrometry from a bacterial or fungal sample with a database of profiles obtained from several characterized microorganisms. However, as the performance of MALDI-TOF MS largely depends on a microorganism's purity and quantity, bacterial enrichment and purification procedures are required from positive blood cultures, which contain high concentrations of interfering non-microbial material118. A retrospective study of 227 cases of S. aureus bacteraemia comparing turnaround time and therapy adjustment before and after the introduction of MALDI-TOF MS plus real-time PCR to detect mecA showed a decrease in turnaround time of MRSA identification by nearly 50% compared with S. aureus identification and β-lactam susceptibility testing by conventional methods. Although the length of hospitalization and rates of adequate empirical antibacterial therapy were similar in the two groups, optimization of therapy occurred more frequently in the group assessed by MALDI-TOF MS119.
Current DNA-based methods for direct MRSA detection from clinical samples are multiplex real-time PCR assays to detect S. aureus and the presence of mecA120 and are well-validated assays121. Results are obtained in approximately 1.5 hours. The FilmArray (Idaho Technology, Salt Lake City, Utah, USA) is a multiplex PCR-based system designed to detect 25 microorganisms (90–95% of the pathogens involved in blood cultures) along with mecA, as well as the presence of genes encoding resistance to vancomycin (vanA and vanB) and carbapenems (blaKPC)122. This assay has higher sensitivity than MALDI-TOF MS in identifying microorganisms from blood culture bottles before positivity, with an average turnaround time of 2.5 hours123.
The application of WGS to bacterial pathogens heralded the single most important advance in diagnostic microbiology and surveillance since in vitro culture. However, direct applications of WGS in diagnostic microbiology remain limited, primarily because of the technological constraints in obtaining results within a time frame that can influence patient care and the need for standardized protocols and automated data interpretation. The introduction of the third generation of sequencers (such as the Oxford Nanopore MinION by Pacific BioSciences and Oxford Nanopore, Oxford, UK) has resulted in longer reads (obtained sequence lengths) that can span repeat regions in the bacterial sequence and enable complete bacterial genome assembly, as well as an increased portability of the machinery and a potential reduction in error rates. An important benefit afforded by the Oxford Nanopore MinION sequencer is that sequencing data can be analysed in real time and could lead to strain identification within 30 min and an antibiotic-resistance profile prediction within 10 hours after the start of a run124, making this assay potentially useful for clinical diagnostics. The utility of WGS has been well demonstrated for studying antibiotic resistance and the population biology of MRSA125 and has also led to many useful insights regarding transmission of MRSA during hospital outbreaks126 and in community settings127.
Screening measures and their effectiveness are discussed in the Prevention section below. Since the introduction of the first MRSA chromogenic medium (that is, a medium containing synthetic chromogenic enzyme substrates; in the presence of the specific target enzyme, the chromogenic substrate is processed and results in a corresponding bacterial colony of a specific colour, thereby enabling pathogen recognition)128, these media have undergone rapid improvements in terms of sensitivity of the chromogen and the antibiotics used120,129. They have become the primary rapid diagnostic assays utilized for active surveillance for MRSA colonization as well as for patient diagnostics since they were introduced in the 2000s129. In 2005, an external quality assessment in 23 European countries and Israel found that 88% of the participating laboratories utilized a chromogenic medium alone to screen for MRSA130. The combination of chromogenic media with MALDI-TOF MS, which enables the species identification of multiple colonies in <1 hour, has further improved the specificity and turnaround time131. Development of automated colony scoring that could further increase specificity and reduce turnaround time is also being attempted132.
Application of real-time PCR-based assays for MRSA screening from nasal swabs can decrease turnaround time to 1–2 hours, whereas the results of chromogenic media-based tests can take a minimum of 14–18 hours without confirmatory testing and, therefore, might not always be useful to guide clinical decisions. An observational cohort study demonstrated a significant reduction in MRSA transmission upon screening with a same-day commercial real-time PCR assay compared with screening with conventional culture (swabs incubated overnight in 7% NaCl and subcultured on mannitol salt agar with 2 milligrams per litre oxacillin for 48 hours): MRSA transmission was 4.9 new acquisitions per 1,000 patient bed days with real-time PCR compared with 13.9 new acquisitions per 1,000 patient bed days with culture133. (A patient bed day represents a unit of time during which a patient occupies a bed and stays overnight in a health-care facility; thus, 50 patients in a hospital over a period of 1 day would represent 50 patient bed days.) However, a major study in 13 ICUs in eight European countries did not find any positive effect of screening using PCR-based tests versus chromogenic media in the acquisition and transmission rates of multidrug-resistant bacteria (including MRSA, vancomycin-resistant enterococci and highly-resistant Enterobacteriaceae)134. Similarly, a UK-based study assessing screening by real-time PCR-based tests versus slower laboratory-based methods (MRSA-selective broth and chromogenic medium) reported a significant reduction in turnaround times (from 40.4 to 3.7 hours) but again no effect on MRSA acquisition rates135, thereby rendering the utility of the more-expensive albeit faster PCR-based screening questionable.
MRSA control interventions have been widely implemented across health-care facilities. These interventions aim to limit the emergence of MRSA by facilitating judicious use of antimicrobial agents (including introducing restrictions on their prescription), control the reservoir of patients who are carriers, prevent MRSA transmission between patients and prevent the development of infection in carriers. Several measures are usually required to successfully prevent transmission and infection with MRSA136. Decolonization, an important control intervention for which there is growing evidence, is discussed in the Management section.
Hand hygiene. By contact with patients with MRSA colonization or handling MRSA-contaminated equipment, health-care workers can acquire MRSA on their hands, and by this means, MRSA can be transmitted between patients137. Hand hygiene, with alcohol-based hand rub or soap and water, aims to reduce MRSA spread via this route. Indeed, the WHO has identified hand hygiene as an important factor in providing safe patient care and has issued detailed instructions regarding appropriate hand hygiene practices among health-care workers137,138. The effectiveness of improving compliance with hand hygiene among health-care workers in MRSA control has been demonstrated at local as well as national levels139,140. For example, the roll out of a national hand hygiene programme in England and Wales from late 2004 was associated with a fall in the incidence of MRSA bacteraemia from 1.88 to 0.91 per 10,000 patient bed days140. Although the hand hygiene campaign was implemented with other national infection control initiatives, the higher procurement of alcohol hand rub during the campaign was independently associated with reduction in the incidence of MRSA bacteraemia after adjustment for all other interventions140.
Active surveillance. Most patients with MRSA colonization are asymptomatic, and, therefore, relying on culture of clinical samples (which are collected only when an individual develops symptoms or signs of infection) alone to identify carriers of MRSA may fail to identify up to 85% of individuals with MRSA colonization141. Through screening methods, active surveillance programmes can identify this large asymptomatic reservoir of carriers and direct interventions (such as topical decolonization) to reduce transmission or infection risk. MRSA screening may be universal (applied to all patients) or targeted (limited to patients at increased risk of MRSA carriage). Universal MRSA screening has been one of the most controversial areas in infection control since the 2000s, with some studies showing that it is effective in reducing MRSA-associated disease142, whereas other studies found it ineffective143,144. Importantly, recent data also show that universal screening is unlikely to be cost-effective, particularly in settings with low or decreasing MRSA prevalence145. On the basis of this accumulating evidence, many health-care facilities have now abandoned universal MRSA screening. We suggest, however, that changes in practices should be based on careful consideration of local MRSA epidemiology and the vulnerability of the patient population.
Randomized trials in ICUs have questioned the utility of routine MRSA screening in this high-risk setting146,147. However, a long turnaround time for screening results (a mean of 5.2 days with a culture-based method using a pre-enrichment step at a central laboratory)146 or established good hand hygiene practices coupled with universal chlorhexidine bathing147 might have contributed to the observed lack of effect of screening. It is argued that ‘horizontal’ strategies (that is, strategies aimed at preventing all health-care-associated infections, including MRSA, such as hand hygiene and universal bathing with antiseptics) are a better use of limited resources.
Contact precautions and isolation. In many facilities, health-care workers use contact precautions (use of disposable gowns and gloves) when caring for patients with MRSA colonization to reduce MRSA transmission associated with contamination of hands and clothing. Although the evidence for this intervention has previously been of low quality, there is now more robust data suggesting that this practice is associated with reduction in MRSA acquisition148. It is also widely recommended that patients with MRSA colonization are isolated in single rooms. However, in a prospective study in an ICU setting where MRSA was endemic and hand hygiene compliance was low, single-room isolation was not effective in reducing MRSA transmission149. Experts have called for a review of this practice and for guidelines to highlight the uncertainties regarding its value150.
The approach to the management of MRSA varies in different geographical regions depending on local MRSA prevalence and availability of antimicrobials, particularly the newer agents.
Decolonization of carriers
MRSA colonization is associated with an increased risk of infection and contributes to transmission. Both MRSA colonization on admission as well as acquisition during hospitalization are associated with an approximately tenfold increased risk of subsequent infection107. Thus, decolonization can contribute to MRSA control by reducing transmission and infection risk. Most decolonization strategies use topical agents applied to the nostrils, the principal site of colonization47. Mupirocin (pseudomonic acid A, which inhibits bacterial isoleucyl tRNA synthetase, preventing protein synthesis) is the principal agent and is often combined with chlorhexidine bathing151. Although mupirocin is the cornerstone for eradication of S. aureus, resistance is increasing, with some studies reporting resistance rates of up to 80% in MRSA152. Alternative agents are being studied, but to date, experience with these agents is limited153. Thus, it is recommended that mupirocin is used judiciously and that the emergence of resistance is monitored152. Ongoing research into the development and evaluation of new agents that can be effectively used for decolonization is also needed.
Short-term decolonization. Decolonization is most commonly used as a protective strategy during relatively short periods of increased risk of infection, for example, during the peri-operative period or ICU stays. Topical mupirocin to the nares and chlorhexidine body washing before surgery for known S. aureus carriers reduced the risk of post-surgical S. aureus infection by ∼50% in a placebo-controlled study154. A subsequent cost-effectiveness analysis using these data showed that the mean cost saved per treated carrier was €1,911 (Ref.155). However, this study was performed in the Netherlands, a country with low MRSA prevalence, and the effects of this short-term decolonization strategy might be different in settings with high MRSA prevalence.
The results of short-term decolonization interventions in the ICU setting have been variable. A large cluster-randomized trial compared three strategies156: screening and isolation of MRSA carriers (no decolonization); a combination of screening, isolation and decolonization (with mupirocin and chlorhexidine bathing) of MRSA carriers (targeted decolonization); and decolonization of all patients (universal decolonization). No significant differences in MRSA colonization and infection rates were found with the three strategies. However, bloodstream infections from any pathogen were significantly lower in the universal decolonization group. This may have been the result of universal chlorhexidine bathing rather than mupirocin. The authors concluded that universal decolonization was the best approach, as it reduced infections overall without the need for screening. However, as widespread use of topical antibiotics might lead to an increase in drug resistance, their use should be coupled with monitoring for resistance152.
Permanent decolonization. In some situations, permanent MRSA eradication is pursued. Permanent decolonization is a component of the ‘search and destroy strategy’ in countries with a low MRSA prevalence157. For example, the Dutch protocol distinguishes between uncomplicated and complicated carriers on the basis of MRSA strain and host characteristics, as well as colonization site, as treatment failure is three times more likely in individuals with throat colonization than in those without throat colonization158. Of 613 MRSA carriers, 80% were ultimately successfully decolonized, with a median time to decolonization of 10 days; of note, adherence to the protocol was crucial for success. Many other clinical trials evaluating permanent decolonization strategies have been conducted under real-life conditions, with rather disappointing results because of a high rate of endogenous recolonization151.
Treatment of symptomatic infection
Empirical treatment and SSTIs. We recommend that an antibiotic effective against MRSA should be considered for empirical treatment of infection for patients with several risk factors for HA-MRSA infection or those with presumed severe staphylococcal infections in settings where MRSA prevalence is >20%, although precise thresholds have not been established. The choice, route of administration and duration of antibiotic therapy are determined by the site and severity of infection. Treatment should then be adjusted on the basis of subsequent results of cultures and susceptibility testing.
Intravenous vancomycin, daptomycin or linezolid can be used for severe SSTIs. Oral therapy as a rule should be avoided in the initial treatment of severe infections. Clindamycin, trimethoprim–sulfamethoxazole and doxycycline are alternative choices for the treatment of mild to moderate SSTIs, depending upon the antibiotic susceptibility testing. For uncomplicated skin abscesses, the use of clindamycin or trimethoprim–sulfamethoxazole in conjunction with incision and drainage has been shown to improve clinical cure rates in the emergency department and other outpatient settings159,160.
Systemic and severe infections. The current recommendations for clinical management of severe MRSA infections include intravenous vancomycin or daptomycin for bacteraemia and intravenous vancomycin or linezolid for hospital-acquired pneumonia161. For severe infections, oral linezolid should not be used for initial therapy. However, when the patient has become stable and can tolerate the oral route, a switch to oral linezolid is recommended. In the setting of infection related to the presence of a medical device (such as central venous catheters), successful treatment usually requires removal of the device when possible161.
Glycopeptides (such as vancomycin and teicoplanin) have been the mainstay of intravenous treatment for MRSA infections. Vancomycin remains the cornerstone of empirical treatment for systemic infections potentially caused by MRSA, first because of its safety profile and second owing to lack of other fully approved alternatives161,162. Teicoplanin is also commonly used in Europe and has been found to be non-inferior to vancomycin in terms of all-cause mortality, with an improved safety profile, although few patients with serious infections were studied163 (Table 3). Of note, glycopeptides have slower bactericidal activity than β-lactam agents, and penetration into tissues is poor.
Recommendations have been made to increase vancomycin administration to achieve an appropriate ‘trough’ concentration (lowest concentration reached by the drug before the next dose is administered) and, in this way, to maximize the chances of microbiological and clinical cure (eradication of the organism as demonstrated by negative cultures and resolution of signs and symptoms of infection, respectively)161,164. Also, optimization of vancomycin therapy on the basis of pharmacokinetic and pharmacodynamic targets is becoming increasingly relevant, particularly as reports of the incidence of MRSA clinical isolates with minimum inhibitory concentrations (MICs) >1 microgram per millilitre (which is just below the breakpoint) are increasing in several settings. However, higher trough concentrations are associated with an increased risk of nephrotoxicity165 and no clear improvement in outcome. Finally, vancomycin is administered in a continuous infusion instead of intermittent injections in some European countries166. However, there are insufficient data to make recommendations regarding this protocol166. In the presence of infections caused by MRSA strains with an MIC higher than the current breakpoint (>2 micrograms per millilitre), vancomycin is not effective, and an alternative agent should be administered167. Switching to daptomycin therapy, on the basis of the daptomycin MIC, should be done as early as possible once an elevated vancomycin MIC is confirmed. Alternative anti-MRSA antibiotics are increasingly being used, but it is important to note that they can have adverse effects, particularly linezolid168 (Table 3). Of note, although reports of vancomycin failure have emerged for vancomycin intermediate-resistant S. aureus (VISA) and/or heterogeneous VISA (hVISA) infections, no data demonstrate superior outcomes with alternative antimicrobials agents (Box 1).
Combination therapy. The duration of bacteraemia in patients with MRSA is twice as long as that in patients with MSSA infection169. The increased duration of bacteraemia is associated with complications (such as attributable mortality, complicated infection, embolic stroke or recurrent S. aureus infection)170. Combination therapy to treat S. aureus (including MRSA) bacteraemia has been used in an attempt to increase bacterial killing, particularly for endocarditis therapy171. However, evidence that combination therapy improves outcomes is lacking171. Several studies have demonstrated in vitro synergy between vancomycin and gentamicin against many MRSA isolates172,173. However, this combination seemed to be numerically inferior to daptomycin alone in the treatment of MRSA bacteraemia and endocarditis in a randomized trial174. Thus, because even low dose gentamicin (1 milligram per kilogram every 8 hours) for a short duration has been associated with substantial nephrotoxicity175 and because the clinical effectiveness of vancomycin plus gentamicin is not confirmed, combination therapy with aminoglycosides is difficult to justify176.
Vancomycin and rifampicin combinations have also been studied, particularly in the context of biofilm infections177. However, the addition of rifampicin to vancomycin is not recommended for MRSA bacteraemia or native valve endocarditis161. In addition, a randomized controlled trial evaluating adjunctive rifampicin in S. aureus (including MRSA) bacteraemia found no overall benefit178.
The combination of vancomycin and β-lactam antibiotics has shown synergistic bacterial killing in vitro179. However, sufficient clinical evidence in favour of this combination is lacking. In the CAMERA-1 trial (comparing vancomycin versus vancomycin plus flucloxacillin), the mean time to resolution of bacteraemia (primary outcome) in the combination group was 1.94 days, compared with 3.00 days in the vancomycin alone group. According to a negative binomial model, the mean time to resolution of bacteraemia in the combination group was 65% (95% CI 41–102%; P = 0.06) of that in the group that received intravenous vancomycin alone (that is, it was 35% lower), and there was no difference between the two groups in relation to the secondary end points179.
Ceftaroline plus daptomycin could be another option for refractory staphylococcal bacteraemia. Ceftaroline offers dual benefit via synergy with daptomycin and sensitization to cathelicidin antimicrobial peptide-derived LL-37, a peptide of the host innate immune response; sensitization to cathelicidin could attenuate the virulence of the pathogen180 (see New drugs and current pipeline). Other combinations (for example, daptomycin and rifampicin) might be promising options in biofilm-related infections181.
Other considerations. In contrast to many other bacterial infections, S. aureus (including MRSA) infections often require a lengthy course of treatment because of the risk of late-onset complications such as abscesses, osteoarticular infection and other secondary foci caused by haematogenous or direct seeding. In cases of documented bacteraemia, the recommended minimum duration of treatment is 14 days161, as short-course therapy is currently not considered to be safe and effective.
Options for salvage therapy, based on low-quality data, include linezolid, trimethoprim–sulfamethoxazole, ceftaroline, quinupristin–dalfopristin and telavancin. Tigecycline should be avoided, as it is bacteriostatic against MRSA and has a large volume of distribution with high concentrations in tissues but low concentrations in serum161. No data in MRSA bacteraemia are yet available for other recently approved agents (for example, ceftobiprole, dalbavancin, oritavancin or tedizolid).
New drugs and current pipeline
Several new agents have been approved for the treatment of SSTIs and in some cases for pneumonia (Fig. 5; Table 4). However, the efficacy and safety of these antibiotics for invasive infections, for which there is a real need, have largely not been demonstrated. The new treatment options have some advantages over older agents and will probably play a part in the therapy of severe MRSA infections in the near future.
Ceftaroline and ceftobiprole are the first β-lactams with anti-MRSA activity. Use of the combination of daptomycin with an anti-staphylococcal β-lactam for refractory MRSA infections has been increasing. Multiple case reports have now documented success of the daptomycin–ceftaroline combination for MRSA bacteraemia and endocarditis182. Ceftobiprole for endocarditis has been studied in animal models only, with promising results183, with a single human case report of ceftobiprole plus daptomycin for MRSA endocarditis184. However, resistance to ceftaroline has been observed in MRSA strains185,186. Of particular concern are reports of resistance in clinical MRSA isolates from patients in geographical regions never exposed to the drug187.
Teicoplanin, introduced in Europe in 1988, was the first natural agent of the lipoglycopeptides class. Synthetic and semisynthetic derivatives of lipoglycopeptides have been produced, including telavancin in 2009 and dalbavancin and oritavancin in 2014 (Ref.188). In 10 years of dalbavancin surveillance testing, only 0.35% of S. aureus isolates exceeded the FDA susceptibility breakpoint and, therefore, were dalbavancin nonsusceptible189. However, the long half-life of dalbavancin could lead to prolonged periods of low-level drug exposure at the end of therapy, potentially increasing the risk of resistance selection190.
Possible advantages of tedizolid over linezolid include once-daily dosing, better adverse effects profile and lower risk of development of spontaneous resistance and susceptibility to the ribosomal RNA large subunit methyltransferase Cfr mobile resistance mechanism. As experience increases, tedizolid may be an attractive alternative for long-term treatment of osteoarticular and central nervous system infections. Trials in pneumonia are underway.
Ceftaroline, ceftobiprole, telavancin, dalbavancin and delafloxacin all require renal dose adjustment (that is, the antibiotic dose requires modification in individuals with impaired renal function).
Quality of life
MRSA infections frequently complicate medical care and cause important treatment challenges. Most experts agree that β-lactam antibiotics are the optimal choice for treating invasive staphylococcal infections171. Thus, MRSA treatment relies on less efficacious (vancomycin) or more expensive (daptomycin or linezolid) therapeutic options. Owing to important prognostic cofactors such as potentially inadequate treatment, patient comorbidities and underlying illness, MRSA infections tend to have higher morbidity and mortality than MSSA infections191.
However, the true clinical effect of methicillin resistance in S. aureus infection has been overestimated owing to methodological shortcomings of studies192. More-recent studies using advanced analytical approaches accounting for potential confounders and competing events confirm a non-negligible effect, which is, however, less pronounced than previously hypothesized193,194. For instance, a large international retrospective cohort study in ten European hospitals with endemic MRSA reported that methicillin resistance in S. aureus bacteraemia was not significantly associated with increased probability of in-hospital mortality (adjusted HR 1.26; 95% CI 0.82–1.94) after adjusting for potential confounders and accounting for the timing of events195. In this study, both MSSA and MRSA bacteraemia led to prolonged length of hospital stay, with a nonsignificant difference of 2.5 days (95% CI –3.2 to 8.3) longer for patients with MRSA infection.
Among patients with bacteraemia caused by S. aureus, methicillin resistance is associated with adverse health outcomes. Several studies show that patients with invasive MRSA infection might have diminished probability of long-term survival, regardless of the adequacy of initial treatment191,196. Furthermore, patients with MRSA infection can experience post-infection sequelae (such as the requirement for amputation owing to the higher risk of treatment failure for MRSA infections of prosthetic joints) and harmful adverse effects related to MRSA treatment197,198. Family members might be overwhelmed with caring for patients with MRSA infection in the community199. By contrast, MRSA carriage may not cause major concern per se, as shown in a Dutch study in which health-related quality of life was not decreased in otherwise healthy pig farmers carrying LA-MRSA200.
Burden of disease
MRSA infections add to the global burden of antibiotic resistance. Several studies have shown that increased incidence of HA-MRSA infection occurs in addition to infections caused by MSSA, increasing the total burden of disease201. Furthermore, once endemic levels of MRSA are reached in a clinical setting, physicians are required to treat patients empirically for MRSA in cases of severe nosocomial infection161. This probabilistic approach of adding vancomycin or linezolid to empiric antibiotic coverage might be continued for years, even after MRSA incidence has substantially declined202. Finally, MRSA control requires substantial infrastructure and productivity costs of surveillance, screening and isolation of MRSA carriers203. However, these MRSA control expenditures (for example, universal, nation-wide MRSA screening) may no longer be justified once MRSA prevalence has declined below specific thresholds145.
The development of a vaccine could have an enormous effect on the incidence and outcome of MRSA infections. Indeed, S. aureus carriers have more frequent infections, but the infections are less severe than those developed by non-carriers204, indicating that long-term exposure to S. aureus antigens can lead to protective immunity. A vaccine could prevent infections at the onset and would ideally also impair S. aureus colonization, thereby strongly reducing the need for antibiotic treatment and extensive infection control measures205. Therapeutic monoclonal antibodies such as the passive vaccine against α-haemolysin by Medimmune (Gaithersburg, Maryland, USA) could provide new treatment opportunities, either alone or in combination with antibiotics. However, despite extensive research and development efforts, a protective vaccine against S. aureus will not become available in the next few years.
Two monovalent vaccine candidates have previously been tested but failed to induce protective immunity in late clinical development. The StaphVax vaccine (Nabi Biopharmaceuticals, Rockville, Maryland, USA), containing the capsular polysaccharide 5 (CP5) and CP8 antigens, and the V710 (Merck, Kenilworth, New Jersey, USA) vaccine, containing the iron-regulated surface determinant protein B (IsdB) antigen, have been protective in animal models but not in placebo-controlled phase III trials206,207. The reasons for failure remain unclear but may be related to the fact that several important S. aureus clones, including the major MRSA clone USA300, do not express any CPs, that the antigen preparations lacked adjuvants and that immune responses to the antigens used were not consistent enough. Moreover, there is a general concern that the extensive set of S. aureus immune evasion factors, such as immunoglobulin G (IgG)-binding protein A, could compromise the efficacy of antibodies, that opsonizing antibodies might not be sufficient to promote protection, whereas toxin-neutralizing antibodies might be equally or even more important, and that appropriate T cell-mediated immunity might be more crucial than previously thought208.
Advances from basic science provide cues for new and hopefully more-successful vaccination approaches. Immunoproteomics studies have helped to elucidate the most immunogenic and protective S. aureus antigens209, and the cell wall glycopolymer wall teichoic acid (WTA) has been identified as a dominant surface antigen210. Several new toxins, whose neutralization by antibodies might contribute to protection, have been identified64. Moreover, it has become clearer which T cell subsets are required for anti-S. aureus immunity211. Pharmaceutical companies continue to develop polyvalent anti-S. aureus vaccines based on surface proteins (ClfA) and polysaccharides (CP5 and CP8), secreted toxins (α-toxin, LukS-PV, ESAT-6 secretion system extracellular protein A (EsxA) and EsxB) and membrane-bound lipoproteins involved in nutrient uptake (manganese transport system membrane protein MntC and ferric hydroxamate receptor 2 (Fhud2))205. An innovative WTA-targeting monoclonal antibody conjugated to a rifampicin-related antibiotic showed protection in preclinical infection models212. There is hope that some of the ongoing vaccine development efforts may lead to successful completion of clinical trials.
Research needs and priorities
MRSA will probably always coexist with humanity. Despite the current focus on multidrug-resistant Gram-negative bacteria and the decline of HA-MRSA infections in some regions, the biomedical research community would be well advised not to abandon its diverse activities in the field of MRSA research. As highlighted by a 2017 WHO report213, MRSA remains among the high-priority multidrug-resistant organisms that need renewed efforts for the research and development of new antibiotics and innovative preventive approaches. In addition to protective vaccines, bacteriophages or bacteriophage-derived lytic proteins could be used for new protective strategies, for instance, for nasal MRSA decolonization in an era of increasing mupirocin resistance214. Overall, there are still many knowledge gaps and important challenges to tackle (Box 2), which require ongoing attention from researchers, policy makers and funders as well as those responsible for MRSA treatment and control.
MRSA has demonstrated its remarkable ability to evolve and disseminate widely in the 60 years since it was first recognized. Several factors, including a better understanding of the pathogenesis of infection, accurate and rapid diagnostics, ensuring the availability of effective treatment options and optimization of the prevention of transmission and infection, will ultimately facilitate control of this highly successful pathogen.
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Nature Reviews Disease Primers would like to thank L. Cui, P. Wilson and other anonymous reviewer(s) for their contribution to the peer review of this work.
Wertheim, H. F. et al. The role of nasal carriage in Staphylococcus aureus infections. Lancet Infect. Dis. 5, 751–762 (2005).
Becker, K. et al. Staphylococcus aureus from the German general population is highly diverse. Int. J. Med. Microbiol. 307, 21–27 (2017).
Kuehnert, M. J. et al. Prevalence of Staphylococcus aureus nasal colonization in the United States, 2001–2002. J. Infect. Dis. 193, 172–179 (2006).
Lowy, F. D. Staphylococcus aureus infections. N. Engi J. Med. 339, 520–532 (1998).
Jevons, M. “Celbenin”-resistant staphylococci. BMJ 1, 124–125 (1961).
Dzintars, K. in Kucers’ The Use of Antibiotics (eds Grayson, M. et al.) 136–142 (CRC Press, 2018).
Chambers, H. F. & Deleo, F. R. Waves of resistance: Staphylococcus aureus in the antibiotic era. Nat. Rev. Microbiol. 7, 629–641 (2009). This is an in-depth review of the clinical and molecular epidemiology of S. aureus, including MRSA, with an emphasis on CA-MRSA.
Faoagali, J. L., Thong, M. L. & Grant, D. Ten years’ experience with methicillin-resistant Staphylococcus aureus in a large Australian hospital. J. Hosp. Infect. 20, 113–119 (1992).
Fridkin, S. K. et al. Methicillin-resistant Staphylococcus aureus disease in three communities. N. Engl. J. Med. 352, 1436–1444 (2005).
Voss, A., Loeffen, F., Bakker, J., Klaassen, C. & Wulf, M. Methicillin-resistant Staphylococcus aureus in pig farming. Emerg. Infect. Dis. 11, 1965–1966 (2005).
Tenover, F. C. et al. Interpreting chromosomal DNA restriction patterns produced by pulsed-field gel electrophoresis: criteria for bacterial strain typing. J. Clin. Microbiol. 33, 2233–2239 (1995).
Ito, T., Katayama, Y. & Hiramatsu, K. Cloning and nucleotide sequence determination of the entire mec DNA of pre-methicillin-resistant Staphylococcus aureus N315. Antimicrob. Agents Chemother 43, 1449–1458 (1999).
Harkins, C. P. et al. Methicillin-resistant Staphylococcus aureus emerged long before the introduction of methicillin into clinical practice. Genome Biol. 18, 130 (2017).
Diekema, D. J. et al. Survey of infections due to Staphylococcus species: frequency of occurrence and antimicrobial susceptibility of isolates collected in the United States, Canada, Latin America, Europe, and the Western Pacific region for the SENTRY Antimicrobial Surveillance Program, 1997–1999. Clin. Infect. Dis. 32 (Suppl. 2), S114–S132 (2001).
Enright, M. C., Day, N. P., Davies, C. E., Peacock, S. J. & Spratt, B. G. Multilocus sequence typing for characterization of methicillin-resistant and methicillin-susceptible clones of Staphylococcus aureus. J. Clin. Microbiol. 38, 1008–1015 (2000).
Monecke, S. et al. A field guide to pandemic, epidemic and sporadic clones of methicillin-resistant Staphylococcus aureus. PLoS ONE 6, e17936 (2011).
[No authors listed.] European Antimicrobial Resistance Surveillance Network (EARS-Net). European Centre for Disease Prevention and Controlhttp://ecdc.europa.eu/en/activities/surveillance/EARS-Net/Pages/index.aspx (2018).
Kock, R. et al. Methicillin-resistant Staphylococcus aureus (MRSA): burden of disease and control challenges in Europe. Eurosurveillance 15, 19688 (2010).
Nielsen, K. L. et al. Fitness cost: a bacteriological explanation for the demise of the first international methicillin-resistant Staphylococcus aureus epidemic. J. Antimicrob. Chemother. 67, 1325–1332 (2012).
Rolain, J. M., Abat, C., Brouqui, P. & Raoult, D. Worldwide decrease in methicillin-resistant Staphylococcus aureus: do we understand something? Clin. Microbiol. Infect. 21, 515–517 (2015).
Garcia- Alvarez, L., Dawson, S., Cookson, B. & Hawkey, P. Working across the veterinary and human health sectors. J. Antimicrob. Chemother. 67 (Suppl. 1), Í37–Í49 (2012).
van Alen, S. et al. In the centre of an epidemic: fifteen years of LA-MRSA CC398 at the University Hospital Munster. Vet. Microbiol. 200, 19–24 (2017).
Lozano, C. et al. High prevalence of spa types associated with the clonal lineage CC398 among tetracycline-resistant methicillin-resistant Staphylococcus aureus strains in a Spanish hospital. J. Antimicrob. Chemother. 67, 330–334 (2012).
van Cleef, B. A. et al. Livestock-associated methicillin-resistant Staphylococcus aureus in humans, Europe. Emerg. Infect. Dis. 17, 502–505 (2011).
Larsen, J. et al. Meticillin-resistant Staphylococcus aureus CC398 is an increasing cause of disease in people with no livestock contact in Denmark, 1999 to 2011. Eurosurveillance 20, 30021 (2015).
Hetem, D. J., Bootsma, M. C., Troelstra, A. & Bonten, M. J. Transmissibility of livestock-associated methicillin-resistant Staphylococcus aureus. Emerg. Infect. Dis. 19, 1797–1802 (2013).
Styers, D., Sheehan, D. J., Hogan, P. & Sahm, D. F. Laboratory-based surveillance of current antimicrobial resistance patterns and trends among Staphylococcus aureus: 2005 status in the United States. Ann. Clin. Microbiol. Antimicrob. 5, 2 (2006).
Talan, D. A. et al. Comparison of Staphylococcus aureus from skin and soft-tissue infections in US emergency department patients, 2004 and 2008. Clin. Infect. Dis. 53, 144–149 (2011).
Moran, G. J. et al. Methicillin-resistant S. aureus infections among patients in the emergency department. N. Engl. J. Med. 355, 666–674 (2006).
Seybold, U. et al. Emergence of community-associated methicillin-resistant Staphylococcus aureus USA300 genotype as a major cause of health care-associated blood stream infections. Clin. Infect. Dis. 42, 647–656 (2006).
Popovich, K. J., Weinstein, R. A. & Hota, B. Are community-associated methicillin-resistant Staphylococcus aureus (MRSA) strains replacing traditional nosocomial MRSA strains? Clin. Infect. Dis. 46, 787–794 (2008).
Planet, P. J. et al. Parallel epidemics of community-associated methicillin-resistant Staphylococcus aureus USA300 infection in North and South America. J. Infect. Dis. 212, 1874–1882 (2015).
Von Dach, E. et al. Comparative genomics of community-associated methicillin-resistant Staphylococcus aureus shows the emergence of clone ST8-USA300 in Geneva, Switzerland. J. Infect. Dis. 213, 1370–1379 (2016).
Dantes, R. et al. National burden of invasive methicillin-resistant Staphylococcus aureus infections, United States, 2011. JAMA Intern. Med. 173, 1970–1978 (2013).
Jain, R. et al. Veterans Affairs initiative to prevent methicillin-resistant Staphylococcus aureus infections. N. Engl. J. Med. 364, 1419–1430 (2011).
Lee, G. M. et al. Effect of nonpayment for preventable infections in U. S. hospitals. N. Engl. J. Med. 367, 1428–1437 (2012).
Chen, C. J. & Huang, Y. C. New epidemiology of Staphylococcus aureus infection in Asia. Clin. Microbiol. Infect. 20, 605–623 (2014).
Mendes, R. E. et al. Regional resistance surveillance program results for 12 Asia-Pacific nations (2011). Antimicrob. Agents Chemother. 57, 5721–5726 (2013).
Lai, C. C., Lin, S. H., Sheng, W. H. & Hsueh, P. R. Decrease in the incidence of meticillin-resistant Staphylococcus aureus nosocomial bloodstream infections in Taiwan. Int. J. Antimicrob. Agents 41, 591–592 (2013).
[No authors listed.] Australian Group on Antimicrobial Resistance (AGAR). AGAR Grouphttp://www.agargroup.org.au/ (2018).
Mitchell, B. G., Collignon, P. J., McCann, R., Wilkinson, I. J. & Wells, A. A major reduction in hospital-onset Staphylococcus aureus bacteremia in Australia-12 years of progress: an observational study. Clin. Infect. Dis. 59, 969–975 (2014).
Williamson, D. A., Coombs, G. W. & Nimmo, G. R. Staphylococcus aureus ‘Down Under’: contemporary epidemiology of S. aureus in Australia, New Zealand, and the South West Pacific. Clin. Microbiol. Infect. 20, 597–604 (2014).
Falagas, M. E., Karageorgopoulos, D. E., Leptidis, J. & Korbila, I. P. MRSA in Africa: filling the global map of antimicrobial resistance. PLoS ONE 8, e68024 (2013).
Brink, A., Moolman, J., da Silva, M. C., Botha, M. & National Antibiotic Surveillance Forum. Antimicrobial susceptibility profile of selected bacteraemic pathogens from private institutions in South Africa. S. Afr. Med. J. 97, 273–279 (2007).
Jansen van Rensburg, M. J., Whitelaw, A. C. & Elisha, B. G. Genetic basis of rifampicin resistance in methicillin-resistant Staphylococcus aureus suggests clonal expansion in hospitals in Cape Town, South Africa. BMC Microbiol. 12, 46 (2012).
Zervou, F. N., Zacharioudakis, I. M., Ziakas, P. D., Rich, J. D. & Mylonakis, E. Prevalence of and risk factors for methicillin-resistant Staphylococcus aureus colonization in HIV infection: a meta-analysis. Clin. Infect. Dis. 59, 1302–1311 (2014).
Kluytmans, J., van Belkum, A. & Verbrugh, H. Nasal carriage of Staphylococcus aureus: epidemiology, underlying mechanisms, and associated risks. Clin. Microbiol. Rev. 10, 505–520 (1997). This is a comprehensive review of staphylococcal nasal colonization including its clinical relevance.
Sim, B. L., McBryde, E., Street, A. C. & Marshall, C. Multiple site surveillance cultures as a predictor of methicillin-resistant Staphylococcus aureus infections. Infect. Control Hosp. Epidemiol. 34, 818–824 (2013).
Eriksen, N. H., Espersen, F., Rosdahl, V. T. & Jensen, K. Carriage of Staphylococcus aureus among 104 healthy persons during a 19-month period. Epidemiol. Infect. 115, 51–60 (1995).
Hoffler, U., Bulanda, M., Heczko, P. B. & Pulverer, G. A comparison of staphylococcal nasal carrier rates in Germany and Poland. Med. Microbiol. Immunol. 164, 285–290 (1978).
Emonts, M. et al. Host polymorphisms in interleukin 4, complement factor H, and C-reactive protein associated with nasal carriage of Staphylococcus aureus and occurrence of boils. J. Infect. Dis. 197, 1244–1253 (2008).
Lucet, J. C. et al. Carriage of methicillin-resistant Staphylococcus aureus in home care settings: prevalence, duration, and transmission to household members. Arch. Intern. Med. 169, 1372–1378 (2009).
Burian, M. et al. Temporal expression of adhesion factors and activity of global regulators during establishment of Staphylococcus aureus nasal colonization. J. Infect. Dis. 201, 1414–1421 (2010).
Weidenmaier, C. et al. Differential roles of sortase-anchored surface proteins and wall teichoic acid in Staphylococcus aureus nasal colonization. Int. J. Med. Microbiol. 298, 505–513 (2008).
Wertheim, H. F. et al. Key role for clumping factor B in Staphylococcus aureus nasal colonization of humans. PLoS Med. 5, e17 (2008).
O’Brien, L. M., Walsh, E. J., Massey, R. C., Peacock, S. J. & Foster, T. J. Staphylococcus aureus clumping factor B (ClfB) promotes adherence to human type I cytokeratin 10: implications for nasal colonization. Cell. Microbiol. 4, 759–770 (2002).
Liu, C. M. et al. Staphylococcus aureus and the ecology of the nasal microbiome. Sci. Adv. 1, e1400216 (2015).
Lemon, K. P. et al. Comparative analyses of the bacterial microbiota of the human nostril and oropharynx. mBio 1, e00129–10 (2010).
Krismer, B. et al. Nutrient limitation governs Staphylococcus aureus metabolism and niche adaptation in the human nose. PLoS Pathog. 10, e1003862 (2014).
Zipperer, A. et al. Human commensals producing a novel antibiotic impair pathogen colonization. Nature 535, 511–516 (2016).
Kaspar, U. et al. The culturome of the human nose habitats reveals individual bacterial fingerprint patterns. Environ. Microbiol. 18, 2130–2142 (2016).
Krismer, B., Weidenmaier, C., Zipperer, A. & Peschel, A. The commensal lifestyle of Staphylococcus aureus and its interactions with the nasal microbiota. Nat. Rev. Microbiol. 15, 675–687 (2017). This review provides a detailed discussion of the complex interplay between S. aureus and other organisms that form part of the nasal microbiota.
Boyle-Vavra, S. et al. USA300 and USA500 clonal lineages of Staphylococcus aureus do not produce a capsular polysaccharide due to conserved mutations in the cap5 locus. mBio 6, e02585–14 (2015).
Spaan, A. N., van Strijp, J. A. G. & Torres, V. J. Leukocidins: staphylococcal bi-component pore-forming toxins find their receptors. Nat. Rev. Microbiol. 15, 435–447 (2017). This is a comprehensive overview of the various pore-forming protein toxins and their cognate host receptors.
Laabei, M. et al. Predicting the virulence of MRSA from its genome sequence. Genome Res. 24, 839–849 (2014).
Thammavongsa, V., Kim, H. K., Missiakas, D. & Schneewind, O. Staphylococcal manipulation of host immune responses. Nat. Rev. Microbiol. 13, 529–543 (2015).
Recker, M. et al. Clonal differences in Staphylococcus aureus bacteraemia-associated mortality. Nat. Microbiol. 2, 1381–1388 (2017). This paper reveals how different S. aureus lineages have adopted different strategies to overcome host responses and cause severe pathology.
Kluytmans, J. A. et al. Nasal carriage of Staphylococcus aureus as a major risk factor for wound infections after cardiac surgery. J. Infect. Dis. 171, 216–219 (1995).
von Eiff, C., Becker, K., Machka, K., Stammer, H. & Peters, G. Nasal carriage as a source of Staphylococcus aureus bacteremia. N. Engl. J. Med. 344, 11–16 (2001).
Foster, T. J., Geoghegan, J. A., Ganesh, V. K. & Hook, M. Adhesion, invasion and evasion: the many functions of the surface proteins of Staphylococcus aureus. Nat. Rev. Microbiol. 12, 49–62 (2014).
Vanhommerig, E. et al. Comparison of biofilm formation between major clonal lineages of methicillin resistant Staphylococcus aureus. PLoS ONE 9, e104561 (2014).
Spaan, A. N., Surewaard, B. G., Nijland, R. & van Strijp, J. A. Neutrophils versus Staphylococcus aureus: a biological tug of war. Annu. Rev. Microbiol. 67, 629–650 (2013).
Hanzelmann, D. et al. Toll-like receptor 2 activation depends on lipopeptide shedding by bacterial surfactants. Nat. Commun. 7, 12304 (2016).
Cheng, A. G., DeDent, A. C., Schneewind, O. & Missiakas, D. A play in four acts: Staphylococcus aureus abscess formation. Trends Microbiol. 19, 225–232 (2011).
Laarman, A., Milder, F., van Strijp, J. & Rooijakkers, S. Complement inhibition by gram-positive pathogens: molecular mechanisms and therapeutic implications. J. Mol. Med. 88, 115–120 (2010).
Stapels, D. A. et al. Staphylococcus aureus secretes a unique class of neutrophil serine protease inhibitors. Proc. Natl Acad. Sci. USA 111, 13187–13192 (2014).
Peschel, A. & Sahl, H. G. The co-evolution of host cationic antimicrobial peptides and microbial resistance. Nat. Rev. Microbiol. 4, 529–536 (2006).
Loffler, B. et al. Staphylococcus aureus panton–valentine leukocidin is a very potent cytotoxic factor for human neutrophils. PLoS Pathog. 6, e1000715 (2010).
Spaulding, A. R. et al. Staphylococcal and streptococcal superantigen exotoxins. Clin. Microbiol. Rev. 26, 422–447 (2013).
Chavakis, T., Wiechmann, K., Preissner, K. T. & Herrmann, M. Staphylococcus aureus interactions with the endothelium: the role of bacterial “secretable expanded repertoire adhesive molecules” (SERAM) in disturbing host defense systems. Thromb. Haemost. 94, 278–285 (2005).
Weidenmaier, C. et al. Lack of wall teichoic acids in Staphylococcus aureus leads to reduced interactions with endothelial cells and to attenuated virulence in a rabbit model of endocarditis. J. Infect. Dis. 191, 1771–1777 (2005).
Loffler, B., Tuchscherr, L., Niemann, S. & Peters, G. Staphylococcus aureus persistence in non-professional phagocytes. Int. J. Med. Microbiol. 304, 170–176 (2014).
Thomer, L., Schneewind, O. & Missiakas, D. Pathogenesis of Staphylococcus aureus bloodstream infections. Annu. Rev. Pathol. 11, 343–364 (2016).
Le, K. Y. & Otto, M. Quorum-sensing regulation in staphylococci-an overview. Front. Microbiol. 6, 1174 (2015).
Cheung, G. Y., Wang, R., Khan, B. A., Sturdevant, D. E. & Otto, M. Role of the accessory gene regulator agr in community-associated methicillin-resistant Staphylococcus aureus pathogenesis. Infect. Immun. 79, 1927–1935 (2011).
Kaito, C. et al. Mobile genetic element SCCmec-encoded psm-mec RNA suppresses translation of agrA and attenuates MRSA virulence. PLoS Pathog. 9, e1003269 (2013).
Painter, K. L., Krishna, A., Wigneshweraraj, S. & Edwards, A. M. What role does the quorum-sensing accessory gene regulator system play during Staphylococcus aureus bacteremia? Trends Microbiol. 22, 676–685 (2014).
Crisostomo, M. I. et al. The evolution of methicillin resistance in Staphylococcus aureus: similarity of genetic backgrounds in historically early methicillin-susceptible and -resistant isolates and contemporary epidemic clones. Proc. Natl Acad. Sci. USA 98, 9865–9870 (2001).
International Working Group on the Classification of Staphylococcal Cassette Chromosome Elements (IWG-SCC). Classification of staphylococcal cassette chromosome mec (SCCmec): guidelines for reporting novel SCCmec elements. Antimicrob. Agents Chemother. 53, 4961–4967 (2009). This paper describes the main SCCmec types and the nomenclature to be followed for the naming of new SCCmec types.
Bal, A. M. et al. Genomic insights into the emergence and spread of international clones of healthcare-, community- and livestock-associated meticillin-resistant Staphylococcus aureus: Blurring of the traditional definitions. J. Glob. Antimicrob. Resist 6, 95–101 (2016).
Hartman, B. J. & Tomasz, A. Low-affinity penicillin-binding protein associated with beta-lactam resistance in Staphylococcus aureus. J. Bacteriol. 158, 513–516 (1984).
Garcia-Alvarez, L. et al. Meticillin-resistant Staphylococcus aureus with a novel mecA homologue in human and bovine populations in the UK and Denmark: a descriptive study. Lancet Infect. Dis. 11, 595–603 (2011).
Kim, C. et al. Properties of a novel PBP2A protein homolog from Staphylococcus aureus strain LGA251 and its contribution to the beta-lactam-resistant phenotype. J. Biol. Chem. 287, 36854–36863 (2012).
Milheirico, C., de Lencastre, H. & Tomasz, A. Full-genome sequencing identifies in the genetic background several determinants that modulate the resistance phenotype in methicillin-resistant Staphylococcus aureus strains carrying the novel mecC gene. Antimicrob. Agents Chemother. 61, e02500–16 (2017).
Becker, K. et al. Plasmid-encoded transferable mecB-mediated methicillin resistance in Staphylococcus aureus. Emerg. Infect. Dis. 24, 242–248 (2018).
Hiramatsu, K., Asada, K., Suzuki, E., Okonogi, K. & Yokota, T. Molecular cloning and nucleotide sequence determination of the regulator region of mecA gene in methicillin-resistant Staphylococcus aureus (MRSA). FEBSLett. 298, 133–136 (1992).
Arede, P., Milheirico, C., de Lencastre, H. & Oliveira, D. C. The anti-repressor MecR2 promotes the proteolysis of the mecA repressor and enables optimal expression of beta-lactam resistance in MRSA. PLoS Pathog. 8, e1002816 (2012).
Zhang, H. Z., Hackbarth, C. J., Chansky, K. M. & ≈Chambers, H. F. A proteolytic transmembrane signaling pathway and resistance to beta-lactams in staphylococci. Science 291, 1962–1965 (2001).
De Lencastre, H. et al. Antibiotic resistance as a stress response: complete sequencing of a large number of chromosomal loci in Staphylococcus aureus strain COL that impact on the expression of resistance to methicillin. Microb. Drug Resist 5, 163–175 (1999).
Kim, C. et al. The mechanism of heterogeneous beta-lactam resistance in MRSA: key role of the stringent stress response. PLoS ONE 8, e82814 (2013).
Boyle-Vavra, S., Yin, S. & Daum, R. S. The VraS/VraR two-component regulatory system required for oxacillin resistance in community-acquired methicillin-resistant Staphylococcus aureus. FEMS Microbiol. Lett. 262, 163–171 (2006).
Jousselin, A. et al. The Staphylococcus aureus chaperone PrsA is a new auxiliary factor of oxacillin resistance affecting penicillin-binding protein 2A. Antimicrob. Agents Chemother 60, 1656–1666 (2015).
Kim, C. K., Milheirico, C., de Lencastre, H. & Tomasz, A. Antibiotic resistance as a stress response: recovery of high-level oxacillin resistance in methicillin-resistant Staphylococcus aureus “Auxiliary” (fem) mutants by induction of the stringent stress response. Antimicrob. Agents Chemother 61, e00313-17 (2017).
Gardete, S. & Tomasz, A. Mechanisms of vancomycin resistance in Staphylococcus aureus. J. Clin. Invest. 124, 2836–2840 (2014). This is a comprehensive review of the mechanisms of vancomycin resistance in S. aureus.
Klevens, R. M. et al. Invasive methicillin-resistant Staphylococcus aureus infections in the United States. JAMA 298, 1763–1771 (2007).
Epstein, L. et al. Risk factors for invasive methicillin-resistant Staphylococcus aureus infection after recent discharge from an acute-care hospitalization, 2011–2013. Clin. Infect. Dis. 62, 45–52 (2016).
Davis, K. A., Stewart, J. J., Crouch, H. K., Florez, C. E. & Hospenthal, D. R. Methicillin-resistant Staphylococcus aureus (MRSA) nares colonization at hospital admission and its effect on subsequent MRSA infection. Clin. Infect. Dis. 39, 776–782 (2004).
Francis, J. S. et al. Severe community-onset pneumonia in healthy adults caused by methicillin-resistant Staphylococcus aureus carrying the Panton–Valentine leukocidin genes. Clin. Infect. Dis. 40, 100–107 (2005).
Miller, L. G. et al. Necrotizing fasciitis caused by community-associated methicillin-resistant Staphylococcus aureus in Los Angeles. N. Engl. J. Med. 352, 1445–1453 (2005).
Kazakova, S. V. et al. A clone of methicillin-resistant Staphylococcus aureus among professional football players. N. Engl. J. Med. 352, 468–475 (2005).
Aiello, A. E., Lowy, F. D., Wright, L. N. & Larson, E. L. Meticillin-resistant Staphylococcus aureus among US prisoners and military personnel: review and recommendations for future studies. Lancet Infect. Dis. 6, 335–341 (2006).
Drougka, E. et al. A 12-year survey of methicillin-resistant Staphylococcus aureus infections in Greece: ST80-IV epidemic? Clin. Microbiol. Infect. 20, O796–803 (2014).
Clinical and Laboratory Standards Institute. M100-S23. Performance Standards for Antimicrobial Susceptibility Testing; Twenty-Third Informational Supplement (CLSI, 2013).
Ryffel, C., Strassle, A., Kayser, F. H. & Berger-Bachi, B. Mechanisms of heteroresistance in methicillin-resistant Staphylococcus aureus. Antimicrob. Agents Chemother. 38, 724–728 (1994).
Penn, C. et al. Wound infections caused by inducible meticillin-resistant Staphylococcus aureus strains. J. Glob. Antimicrob. Resist 1, 79–83 (2013).
Winstanley, T. & Courvalin, P. Expert systems in clinical microbiology. Clin. Microbiol. Rev. 24, 515–556 (2011). This reference is a good overview of automated systems for the detection of resistance mechanisms with a critical review of published evaluations of the performance of each system.
Bhowmick, T. et al. Controlled multicenter evaluation of a bacteriophage-based method for rapid detection of Staphylococcus aureus in positive blood cultures. J. Clin. Microbiol. 51, 1226–1230 (2013).
Opota, O., Croxatto, A., Prod’hom, G. & Greub, G. Blood culture-based diagnosis of bacteraemia: state of the art. Clin. Microbiol. Infect. 21, 313–322 (2015).
Romero-Gomez, M. P., Cendejas-Bueno, E., Garcia Rodriguez, J. & Mingorance, J. Impact of rapid diagnosis of Staphylococcus aureus bacteremia from positive blood cultures on patient management. Eur. J. Clin. Microbiol. Infect. Dis. 36, 2469–2473 (2017).
Malhotra-Kumar, S. et al. Current trends in rapid diagnostics for methicillin-resistant Staphylococcus aureus and glycopeptide-resistant enterococcus species. J. Clin. Microbiol. 46, 1577–1587 (2008).
Malhotra- Kumar, S. et al. Evaluation of molecular assays for rapid detection of methicillin-resistant Staphylococcus aureus. J. Clin. Microbiol. 48, 4598–4601 (2010).
Blaschke, A. J. et al. Rapid identification of pathogens from positive blood cultures by multiplex polymerase chain reaction using the FilmArray system. Diagnost. Microbiol. Infect. Dis. 74, 349–355 (2012).
Almuhayawi, M., Altun, O., Stralin, K. & Ozenci, V. Identification of microorganisms by FilmArray and matrix-assisted laser desorption ionization-time of flight mass spectrometry prior to positivity in the blood culture system. J. Clin. Microbiol. 52, 3230–3236 (2014).
Cao, M. D. et al. Streaming algorithms for identification of pathogens and antibiotic resistance potential from real-time MinION(TM) sequencing. GigaScience 5, 32 (2016).
Aanensen, D. M. et al. Whole-genome sequencing for routine pathogen surveillance in public health: a population snapshot of invasive Staphylococcus aureus in Europe. mBio 7, e00444-16 (2016).
Koser, C. U. et al. Rapid whole-genome sequencing for investigation of a neonatal MRSA outbreak. N. Engl. J. Med. 366, 2267–2275 (2012).
Millar, E. V. et al. Genomic characterization of USA300 methicillin-resistant Staphylococcus aureus (MRSA) to evaluate intraclass transmission and recurrence of skin and soft tissue infection (SSTI) among high-risk military trainees. Clin. Infect. Dis. 65, 461–468 (2017).
Merlino, J., Leroi, M., Bradbury, R., Veal, D. & Harbour, C. New chromogenic identification and detection of Staphylococcus aureus and methicillin-resistant S. aureus. J. Clin. Microbiol. 38, 2378–2380 (2000).
Perry, J. D. A. Decade of development of chromogenic culture media for clinical microbiology in an era of molecular diagnostics. Clin. Microbiol. Rev. 30, 449–479 (2017). Tqhis is a comprehensive reference reviewing rapid culture methods for the detection of MRSA and other multidrug-resistant organisms.
Gazin, M. et al. Culture-based detection of methicillin-resistant Staphylococcus aureus by a network of European laboratories: an external quality assessment study. Eur. J. Clin. Microbiol. Infect. Dis. 31, 1765–1770 (2012).
Luthje, P. et al. Identification of microorganisms grown on chromogenic media by MALDI-TOF MS. J. Microbiol. Methods 136, 17–20 (2017).
Faron, M. L. et al. Automated scoring of chromogenic media for detection of methicillin-resistant Staphylococcus aureus by use of WASPLab image analysis software. J. Clin. Microbiol. 54, 620–624 (2016).
Cunningham, R. et al. Effect on MRSA transmission of rapid PCR testing of patients admitted to critical care. J. Hosp. Infect. 65, 24–28 (2007).
Derde, L. P. G. et al. Interventions to reduce colonisation and transmission of antimicrobial-resistant bacteria in intensive care units: an interrupted time series study and cluster randomised trial. Lancet Infect. Dis. 14, 31–39 (2014).
Wu, P. J., Jeyaratnam, D., Tosas, O., Cooper, B. S. & French, G. L. Point-of-care universal screening for meticillin-resistant Staphylococcus aureus: a cluster-randomized cross-over trial. J. Hosp. Infect. 95, 245–252 (2017).
Calfee, D. P. et al. Strategies to prevent methicillin-resistant Staphylococcus aureus transmission and infection in acute care hospitals: 2014 update. Infect. Control Hosp. Epidemiol. 35, 772–796 (2014). This paper is an expert guidance document, with grading of the quality of the evidence, for MRSA control in acute care facilities.
World Health Organization. WHO Guidelines on Hand Hygiene in Health Care. World Alliance for Patient Safety (WHO Press, Geneva, 2009).
Sax, H. et al. ‘My five moments for hand hygiene’: a user-centred design approach to understand, train, monitor and report hand hygiene. J. Hosp. Infect. 67, 9–21 (2007).
Pittet, D. et al. Effectiveness of a hospital-wide programme to improve compliance with hand hygiene. Lancet 356, 1307–1312 (2000).
Stone, S. P. et al. Evaluation of the national Cleanyourhands campaign to reduce Staphylococcus aureus bacteraemia and Clostridium difficile infection in hospitals in England and Wales by improved hand hygiene: four year, prospective, ecological, interrupted time series study. BMJ 344, e3005 (2012).
Salgado, C. D. & Farr, B. M. What proportion of hospital patients colonized with methicillin-resistant Staphylococcus aureus are identified by clinical microbiological cultures? Infect. Control Hosp. Epidemiol. 27, 116–121 (2006).
Robicsek, A. et al. Universal surveillance for methicillin-resistant Staphylococcus aureus in 3 affiliated hospitals. Ann. Intern. Med. 148, 409–418 (2008).
Harbarth, S. et al. Universal screening for methicillin-resistant Staphylococcus aureus at hospital admission and nosocomial infection in surgical patients. JAMA 299, 1149–1157 (2008).
Lee, A. S. et al. Comparison of strategies to reduce meticillin-resistant Staphylococcus aureus rates in surgical patients: a controlled multicentre intervention trial. BMJ Open 3, e003126 (2013).
Robotham, J. V. et al. Cost-effectiveness of national mandatory screening of all admissions to English National Health Service hospitals for meticillin-resistant Staphylococcus aureus: a mathematical modelling study. Lancet Infect. Dis. 16, 348–356 (2016).
Huskins, W. C. et al. Intervention to reduce transmission of resistant bacteria in intensive care. N. Engl. J. Med. 364, 1407–1418 (2011).
Derde, L. P. et al. Interventions to reduce colonisation and transmission of antimicrobial-resistant bacteria in intensive care units: an interrupted time series study and cluster randomised trial. Lancet Infect. Dis. 14, 31–39 (2014).
Harris, A. D. et al. Universal glove and gown use and acquisition of antibiotic-resistant bacteria in the ICU: a randomized trial. JAMA 310, 1571–1580 (2013).
Cepeda, J. A. et al. Isolation of patients in single rooms or cohorts to reduce spread of MRSA in intensive-care units: prospective two-centre study. Lancet 365, 295–304 (2005).
Fatkenheuer, G., Hirschel, B. & Harbarth, S. Screening and isolation to control meticillin-resistant Staphylococcus aureus: sense, nonsense, and evidence. Lancet 385, 1146–1149 (2015). This commentary provides an update regarding the growing evidence for and against the role of active surveillance in MRSA control.
Loeb, M., Main, C., Walker-Dilks, C. & Eady, A. Antimicrobial drugs for treating methicillin-resistant Staphylococcus aureus colonization. Cochrane Database Syst. Rev. 4, CD003340 (2003).
Poovelikunnel, T., Gethin, G. & Humphreys, H. Mupirocin resistance: clinical implications and potential alternatives for the eradication of MRSA. J. Antimicrob. Chemother. 70, 2681–2692 (2015).
Landelle, C. et al. Randomized, placebo-controlled, double-blind clinical trial to evaluate the efficacy of polyhexanide for topical decolonization of MRSA carriers. J. Antimicrob. Chemother. 71, 531–538 (2016).
Bode, L. G. et al. Preventing surgical-site infections in nasal carriers of Staphylococcus aureus. N. Engl. J. Med. 362, 9–17 (2010).
van Rijen, M. M., Bode, L. G., Baak, D. A., Kluytmans, J. A. & Vos, M. C. Reduced costs for Staphylococcus aureus carriers treated prophylactically with mupirocin and chlorhexidine in cardiothoracic and orthopaedic surgery. PLoS ONE 7, e43065 (2012).
Huang, S. S. et al. Targeted versus universal decolonization to prevent ICU infection. N. Engl. J. Med. 368, 2255–2265 (2013).
Ammerlaan, H. S. et al. Eradication of carriage with methicillin-resistant Staphylococcus aureus: effectiveness of a national guideline. J. Antimicrob. Chemother. 66, 2409–2417 (2011).
Ammerlaan, H. S. et al. Eradication of carriage with methicillin-resistant Staphylococcus aureus: determinants of treatment failure. J. Antimicrob. Chemother. 66, 2418–2424 (2011).
Talan, D. A. et al. Trimethoprim-sulfamethoxazole versus placebo for uncomplicated skin abscess. N. Engl. J. Med. 374, 823–832 (2016).
Daum, R. S. et al. A placebo-controlled trial of antibiotics for smaller skin abscesses. N. Engl. J. Med. 376, 2545–2555 (2017).
Liu, C. et al. Clinical practice guidelines by the Infectious Diseases Society of America for the treatment of methicillin-resistant Staphylococcus aureus infections in adults and children. Clin. Infect. Dis. 52, e18–55 (2011). This paper represents an essential and up-to-date guidance document for management of MRSA infection.
Gould, I. M. et al. New insights into meticillin-resistant Staphylococcus aureus (MRSA) pathogenesis, treatment and resistance. Int. J. Antimicrob. Agents 39, 96–104 (2012).
Svetitsky, S., Leibovici, L. & Paul, M. Comparative efficacy and safety of vancomycin versus teicoplanin: systematic review and meta-analysis. Antimicrob. Agents Chemother. 53, 4069–4079 (2009).
Vandecasteele, S. J., De Vriese, A. S. & Tacconelli, E. The pharmacokinetics and pharmacodynamics of vancomycin in clinical practice: evidence and uncertainties. J. Antimicrob. Chemother. 68, 743–748 (2013).
Lodise, T. P., Patel, N., Lomaestro, B. M., Rodvold, K. A. & Drusano, G. L. Relationship between initial vancomycin concentration-time profile and nephrotoxicity among hospitalized patients. Clin. Infect. Dis. 49, 507–514 (2009).
Cataldo, M. A., Tacconelli, E., Grilli, E., Pea, F. & Petrosillo, N. Continuous versus intermittent infusion of vancomycin for the treatment of Gram-positive infections: systematic review and meta-analysis. J. Antimicrob. Chemother. 67, 17–24 (2012).
Bradley, J. S. Which antibiotic for resistant Gram-positives, and why? J. Infect. 68 (Suppl. 1), S63–75 (2014).
Falagas, M. E. & Vardakas, K. Z. Benefit-risk assessment of linezolid for serious gram-positive bacterial infections. DrugSaf. 31, 753–768 (2008).
Cosgrove, S. E. et al. Comparison of mortality associated with methicillin-resistant and methicillin-susceptible Staphylococcus aureus bacteremia: a meta-analysis. Clin. Infect. Dis. 36, 53–59 (2003).
Fowler, V. G. Jr. et al. Clinical identifiers of complicated Staphylococcus aureus bacteremia. Arch. Intern. Med. 163, 2066–2072 (2003).
Thwaites, G. E. et al. Clinical management of Staphylococcus aureus bacteraemia. Lancet Infect. Dis. 11, 208–222 (2011). This is an important reference for all persons interested in the optimal treatment of S. aureus bacteraemia.
Houlihan, H. H., Mercier, R. C. & Rybak, M. J. Pharmacodynamics of vancomycin alone and in combination with gentamicin at various dosing intervals against methicillin-resistant Staphylococcus aureus-infected fibrin-platelet clots in an in vitro infection model. Antimicrob. Agents Chemother. 41, 2497–2501 (1997).
Tsuji, B. T. & Rybak, M. J. Short-course gentamicin in combination with daptomycin or vancomycin against Staphylococcus aureus in an in vitro pharmacodynamic model with simulated endocardial vegetations. Antimicrob. Agents Chemother. 49, 2735–2745 (2005).
Rehm, S. J. et al. Daptomycin versus vancomycin plus gentamicin for treatment of bacteraemia and endocarditis due to Staphylococcus aureus: subset analysis of patients infected with methicillin-resistant isolates. J. Antimicrob. Chemother. 62, 1413–1421 (2008).
Fowler, V. G. Jr. et al. Daptomycin versus standard therapy for bacteremia and endocarditis caused by Staphylococcus aureus. N. Engl. J. Med. 355, 653–665 (2006).
Bayer, A. S. & Murray, B. E. Initial low-dose aminoglycosides in Staphylococcus aureus bacteremia: good science, urban legend, or just plain toxic? Clin. Infect. Dis. 48, 722–724 (2009).
Forrest, G. N. & Tamura, K. Rifampin combination therapy for nonmycobacterial infections. Clin. Microbiol. Rev. 23, 14–34 (2010).
Thwaites, G. E. et al. Adjunctive rifampicin for Staphylococcus aureus bacteraemia (ARREST): a multicentre, randomised, double-blind, placebo-controlled trial. Lancet 391, 668–678 (2018).
Davis, J. S. et al. Combination of vancomycin and beta-lactam therapy for methicillin-resistant Staphylococcus aureus bacteremia: a pilot multicenter randomized controlled trial. Clin. Infect. Dis. 62, 173–180 (2016).
Sakoulas, G. et al. Antimicrobial salvage therapy for persistent staphylococcal bacteremia using daptomycin plus ceftaroline. Clin. Ther. 36, 1317–1333 (2014).
Rose, W. E., Berti, A. D., Hatch, J. B. & Maki, D. G. Relationship of in vitro synergy and treatment outcome with daptomycin plus rifampin in patients with invasive methicillin-resistant Staphylococcus aureus infections. Antimicrob. Agents Chemother. 57, 3450–3452 (2013).
Cosimi, R. A., Beik, N., Kubiak, D. W. & Johnson, J. A. Ceftaroline for severe methicillin-resistant Staphylococcus aureus infections: a systematic review. Open Forum Infect. Dis. 4, ofx084 (2017).
Tattevin, P., Basuino, L., Bauer, D., Diep, B. A. & Chambers, H. F. Ceftobiprole is superior to vancomycin, daptomycin, and linezolid for treatment of experimental endocarditis in rabbits caused by methicillin-resistant Staphylococcus aureus. Antimicrob. Agents Chemother. 54, 610–613 (2010).
Oltolini, C. et al. Meticillin-resistant Staphylococcus aureus endocarditis: first report of daptomycin plus ceftobiprole combination as salvage therapy. Int. J. Antimicrob. Agents 47, 502–504 (2016).
Andrey, D. O. et al. Antimicrobial activity of ceftaroline against methicillin-resistant Staphylococcus aureus (MRSA) isolates collected in 2013–2014 at the Geneva University Hospitals. Eur. J. Clin. Microbiol. Infect. Dis. 36, 343–350 (2017).
Long, S. W. et al. PBP2a mutations causing high-level Ceftaroline resistance in clinical methicillin-resistant Staphylococcus aureus isolates. Antimicrob. Agents Chemother. 58, 6668–6674 (2014).
Mendes, R. E. et al. Characterization of methicillin-resistant Staphylococcus aureus displaying increased MICs of ceftaroline. J. Antimicrob. Chemother. 67, 1321–1324 (2012).
Zhanel, G. G. et al. New lipoglycopeptides: a comparative review of dalbavancin, oritavancin and telavancin. Drugs 70, 859–886 (2010).
McCurdy, S. P., Jones, R. N., Mendes, R. E., Puttagunta, S. & Dunne, M. W. In vitro activity of dalbavancin against drug-resistant Staphylococcus aureus isolates from a global surveillance program. Antimicrob. Agents Chemother. 59, 5007–5009 (2015).
Werth, B. J. et al. Emergence of dalbavancin non-susceptible, vancomycin-intermediate Staphylococcus aureus (VISA) after treatment of MRSA central line-associated bloodstream infection with a dalbavancin- and vancomycin-containing regimen. Clin. Microbiol. Infect. 24, 429.e1–429.e5 (2018).
Yaw, L. K., Robinson, J. O. & Ho, K. M. A comparison of long-term outcomes after meticillin-resistant and meticillin-sensitive Staphylococcus aureus bacteraemia: an observational cohort study. Lancet Infect. Dis. 14, 967–975 (2014).
Fatkenheuer, G. & Kaasch, A. J. How deadly is meticillin-resistant Staphylococcus aureus? Lancet Infect. Dis. 14, 905–907 (2014).
De Angelis, G. et al. Multistate modelling to estimate the excess length of stay associated with meticillin-resistant Staphylococcus aureus colonisation and infection in surgical patients. J. Hosp. Infect. 78, 86–91 (2011).
De Angelis, G., Murthy, A., Beyersmann, J. & Harbarth, S. Estimating the impact of healthcare-associated infections on length of stay and costs. Clin. Microbiol. Infect. 16, 1729–1735 (2010).
Stewardson, A. J. et al. The health and economic burden of bloodstream infections caused by antimicrobial-susceptible and non-susceptible Enterobacteriaceae and Staphylococcus aureus in European hospitals, 2010 and 2011: a multicentre retrospective cohort study. Eurosurveillance 21, 30319 (2016). This is a methodologically sound analysis of excess length of stay of MRSA bacteraemia.
Haessler, S., Mackenzie, T. & Kirkland, K. B. Long-term outcomes following infection with meticillin-resistant or meticillin-susceptible Staphylococcus aureus. J. Hosp. Infect. 69, 39–45 (2008).
Pendleton, A. & Kocher, M. S. Methicillin-resistant Staphylococcus aureus bone and joint infections in children. J. Am. Acad. Orthop. Surg. 23, 29–37 (2015).
Salgado, C. D., Dash, S., Cantey, J. R. & Marculescu, C. E. Higher risk of failure of methicillin-resistant Staphylococcus aureus prosthetic joint infections. Clin. Orthop. Relat. Res. 461, 48–53 (2007).
Gleeson, A., Larkin, P. & O'Sullivan, N. The impact of meticillin-resistant Staphylococcus aureus on patients with advanced cancer and their family members: a qualitative study. Palliat. Med. 30, 382–391 (2016).
van Cleef, B. A. et al. Health and health-related quality of life in pig farmers carrying livestock-associated methicillin-resistant Staphylococcus aureus. Epidemiol. Infect. 144, 1774–1783 (2016).
Ammerlaan, H. S. et al. Secular trends in nosocomial bloodstream infections: antibiotic-resistant bacteria increase the total burden of infection. Clin. Infect. Dis. 56, 798–805 (2013). This is most likely the best paper evaluating the question of whether MRSA adds to the overall burden of nosocomial infections.
Jones, B. E. et al. Variation in empiric coverage versus detection of methicillin-resistant Staphylococcus aureus and Pseudomonas aeruginosa in hospitalizations for community-onset pneumonia across 128 US veterans affairs medical centers. Infect. Control Hosp. Epidemiol. 38, 937–944 (2017).
Herr, C. E., Heckrodt, T. H., Hofmann, F. A., Schnettler, R. & Eikmann, T. F. Additional costs for preventing the spread of methicillin-resistant Staphylococcus aureus and a strategy for reducing these costs on a surgical ward. Infect. Control Hosp. Epidemiol. 24, 673–678 (2003).
Wertheim, H. F. et al. Risk and outcome of nosocomial Staphylococcus aureus bacteraemia in nasal carriers versus non-carriers. Lancet 364, 703–705 (2004).
Pozzi, C. et al. Vaccines for Staphylococcus aureus and target populations. Curr. Top. Microbiol. Immunol. 409, 491–528 (2017).
Fowler, V. G. et al. Effect of an investigational vaccine for preventing Staphylococcus aureus infections after cardiothoracic surgery: a randomized trial. JAMA 309, 1368–1378 (2013).
Shinefield, H. et al. Use of a Staphylococcus aureus conjugate vaccine in patients receiving hemodialysis. N. Engl. J. Med. 346, 491–496 (2002).
Fowler, V. G. Jr & Proctor, R. A. Where does a Staphylococcus aureus vaccine stand? Clin. Microbiol. Infect. 20 (Suppl. 5), 66–75 (2014).
Stentzel, S. et al. Specific serum IgG at diagnosis of Staphylococcus aureus bloodstream invasion is correlated with disease progression. J. Proteom. 128, 1–7 (2015).
Kurokawa, K., Takahashi, K. & Lee, B. L. The staphylococcal surface-glycopolymer wall teichoic acid (WTA) is crucial for complement activation and immunological defense against Staphylococcus aureus infection. Immunobiology 221, 1091–1101 (2016).
Bekeredjian-Ding, I. Deciphering the significance of the T cell response to Staphylococcus aureus. Future Microbiol. 12, 1023–1026 (2017).
Lehar, S. M. et al. Novel antibody-antibiotic conjugate eliminates intracellular S. aureus. Nature 527, 323–328 (2015).
World Health Organization. Prioritization of Pathogens to Guide Discovery, Research and Development of New Antibiotics for Drug-Resistant Bacterial Infections, Including Tuberculosis (WHO, Geneva, 2017).
Idelevich, E. A. et al. In vitro activity against Staphylococcus aureus of a novel antimicrobial agent, PRF-119, a recombinant chimeric bacteriophage endolysin. Antimicrob. Agents Chemother. 55, 4416–4419 (2011).
Hiramatsu, K. et al. Methicillin-resistant Staphylococcus aureus clinical strain with reduced vancomycin susceptibility. J. Antimicrob. Chemother. 40, 135–136 (1997).
Mwangi, M. M. et al. Tracking the in vivo evolution of multidrug resistance in Staphylococcus aureus by whole-genome sequencing. Proc. Natl Acad. Sci. USA 104, 9451–9456 (2007).
Howden, B. P., Davies, J. K., Johnson, P. D., Stinear, T. P. & Grayson, M. L. Reduced vancomycin susceptibility in Staphylococcus aureus, including vancomycin-intermediate and heterogeneous vancomycin-intermediate strains: resistance mechanisms, laboratory detection, and clinical implications. Clin. Microbiol. Rev. 23, 99–139 (2010).
Khatib, R. et al. Relevance of vancomycin-intermediate susceptibility and heteroresistance in methicillin-resistant Staphylococcus aureus bacteraemia. J. Antimicrob. Chemother. 66, 1594–1599 (2011).
Satola, S. W. et al. Clinical and laboratory characteristics of invasive infections due to methicillin-resistant Staphylococcus aureus isolates demonstrating a vancomycin MIC of 2 micrograms per milliliter: lack of effect of heteroresistant vancomycin-intermediate S. aureus phenotype. J. Clin. Microbiol. 49, 1583–1587 (2011).
Sievert, D. M. et al. Vancomycin-resistant Staphylococcus aureus in the United States, 2002–2006. Clin. Infect. Dis. 46, 668–674 (2008).
Weigel, L. M. et al. Genetic analysis of a high-level vancomycin-resistant isolate of Staphylococcus aureus. Science 302, 1569–1571 (2003).
Foucault, M. L., Courvalin, P. & Grillot-Courvalin, C. Fitness cost of VanA-type vancomycin resistance in methicillin-resistant Staphylococcus aureus. Antimicrob. Agents Chemother. 53, 2354–2359 (2009).
Stefani, S. et al. Meticillin-resistant Staphylococcus aureus (MRSA): global epidemiology and harmonisation of typing methods. Int. J. Antimicrob. Agents 39, 273–282 (2012).
Carlet, J. et al. French national program for prevention of healthcare-associated infections and antimicrobial resistance, 1992-2008: positive trends, but perseverance needed. Infect. Control Hosp. Epidemiol. 30, 737–745 (2009).
Duerden, B., Fry, C., Johnson, A. P. & Wilcox, M. H. The control of methicillin-resistant Staphylococcus aureus blood stream infections in England. Open Forum Infect. Dis. 2, ofv035 (2015).
[No authors listed.] PubMLST. University of Oxfordhttps://pubmlst.org/ (2018).
Thurlow, L. R., Joshi, G. S. & Richardson, A. R. Virulence strategies of the dominant USA300 lineage of community-associated methicillin-resistant Staphylococcus aureus (CA-MRSA). FEMS Immunol. Med. Microbiol. 65, 5–22 (2012).
Peschel, A. & Otto, M. Phenol-soluble modulins and staphylococcal infection. Nat. Rev. Microbiol. 11, 667–673 (2013).
Wright, G. D. Q&A: Antibiotic resistance: where does it come from and what can we do about it? BMC Biol. 8, 123 (2010).
McCarthy, A. J. & Lindsay, J. A. Staphylococcus aureus innate immune evasion is lineage-specific: a bioinfomatics study. Infect. Genet. Evol. 19, 7–14 (2013).
Markowitz, N., Quinn, E. L. & Saravolatz, L. D. Trimethoprim-sulfamethoxazole compared with vancomycin for the treatment of Staphylococcus aureus infection. Ann. Intern. Med. 117, 390–398 (1992).
Landersdorfer, C. B., Bulitta, J. B., Kinzig, M., Holzgrabe, U. & Sorgel, F. Penetration of antibacterials into bone: pharmacokinetic, pharmacodynamic and bioanalytical considerations. Clin. Pharmacokinet. 48, 89–124 (2009).
Sakoulas, G., Alder, J., Thauvin-Eliopoulos, C., Moellering, R. C. Jr & Eliopoulos, G. M. Induction of daptomycin heterogeneous susceptibility in Staphylococcus aureus by exposure to vancomycin. Antimicrob. Agents Chemother. 50, 1581–1585 (2006).
Pertel, P. E. et al. Effects of prior effective therapy on the efficacy of daptomycin and ceftriaxone for the treatment of community-acquired pneumonia. Clin. Infect. Dis. 46, 1142–1151 (2008).
Fenton, C., Keating, G. M. & Curran, M. P. Daptomycin. Drugs 64, 445–455 (2004).
Pea, F. et al. Therapeutic drug monitoring may improve safety outcomes of long-term treatment with linezolid in adult patients. J. Antimicrob. Chemother. 67, 2034–2042 (2012).
Itani, K. M. et al. Efficacy and safety of linezolid versus vancomycin for the treatment of complicated skin and soft-tissue infections proven to be caused by methicillin-resistant Staphylococcus aureus. Am. J. Surg. 199, 804–816 (2010).
Corey, G. R. et al. CANVAS 1: the first Phase III, randomized, double-blind study evaluating ceftaroline fosamil for the treatment of patients with complicated skin and skin structure infections. J. Antimicrob. Chemother. 65 (Suppl. 4), iv41–iv51 (2010).
Wilcox, M. H. et al. CANVAS 2: the second Phase III, randomized, double-blind study evaluating ceftaroline fosamil for the treatment of patients with complicated skin and skin structure infections. J. Antimicrob. Chemother. 65 (Suppl. 4), iv53–iv65 (2010).
Dryden, M., Zhang, Y., Wilson, D., Iaconis, J. P. & Gonzalez, J. A. Phase III, randomized, controlled, non-inferiority trial of ceftaroline fosamil 600 mg every 8 h versus vancomycin plus aztreonam in patients with complicated skin and soft tissue infection with systemic inflammatory response or underlying comorbidities. J. Antimicrob. Chemother. 71, 3575–3584 (2016).
Noel, G. J., Bush, K., Bagchi, P., Ianus, J. & Strauss, R. S. A randomized, double-blind trial comparing ceftobiprole medocaril with vancomycin plus ceftazidime for the treatment of patients with complicated skin and skin-structure infections. Clin. Infect. Dis. 46, 647–655 (2008).
[No authors listed.] Vibativ (telavancin) [prescribing information]. Astellashttp://www.astellas.us/docs/us/VIBATIV_PI_Final.pdf (2009).
Rubinstein, E. et al. Telavancin versus vancomycin for hospital-acquired pneumonia due to gram-positive pathogens. Clin. Infect. Dis. 52, 31–40 (2011).
Stryjewski, M. E. et al. A randomized Phase 2 trial of telavancin versus standard therapy in patients with uncomplicated Staphylococcus aureus bacteremia: the ASSURE study. BMC Infect. Dis. 14, 289 (2014).
Nord, C. E., Rasmanis, G. & Wahlund, E. Effect of dalbavancin on the normal intestinal microflora. J. Antimicrob. Chemother. 58, 627–631 (2006).
Ramdeen, S. & Boucher, H. W. Dalbavancin for the treatment of acute bacterial skin and skin structure infections. Expert Opin. Pharmacother. 16, 2073–2081 (2015).
Messina, J. A., Fowler, V. G. Jr & Corey, G. R. Oritavancin for acute bacterial skin and skin structure infections. Expert Opin. Pharmacother. 16, 1091–1098 (2015).
Biedenbach, D. J., Arhin, F. F., Moeck, G., Lynch, T. F. & Sahm, D. F. In vitro activity of oritavancin and comparator agents against staphylococci, streptococci and enterococci from clinical infections in Europe and North America, 2011–2014. Int. J. Antimicrob. Agents 46, 674–681 (2015).
Prokocimer, P., De Anda, C., Fang, E., Mehra, P. & Das, A. Tedizolid phosphate versus linezolid for treatment of acute bacterial skin and skin structure infections: the ESTABLISH-1 randomized trial. JAMA 309, 559–569 (2013).
Moran, G. J. et al. Tedizolid for 6 days versus linezolid for 10 days for acute bacterial skin and skin-structure infections (ESTABLISH-2): a randomised, double-blind, phase 3, non-inferiority trial. Lancet Infect. Dis. 14, 696–705 (2014).
Van Bambeke, F. Delafloxacin, a non-zwitterionic fluoroquinolone in Phase III of clinical development: evaluation of its pharmacology, pharmacokinetics, pharmacodynamics and clinical efficacy. Future Microbiol. 10, 1111–1123 (2015).
Kingsley, J. et al. A randomized, double-blind, Phase 2 study to evaluate subjective and objective outcomes in patients with acute bacterial skin and skin structure infections treated with delafloxacin, linezolid or vancomycin. J. Antimicrob. Chemother 71, 821–829 (2016).
Pullman, J. et al. Efficacy and safety of delafloxacin compared with vancomycin plus aztreonam for acute bacterial skin and skin structure infections: a phase 3, double-blind, randomized study. J. Antimicrob. Chemother. 72, 3471–3480 (2017).
H.d.L. thanks A. Tomasz and C. Milheiriço for helpful discussions while preparing the manuscript. H.d.L.'s research is supported by Project LISBOA-01-0145-FEDER-007660 funded by the European Regional Development Fund through COMPETE2020 (POCI) and by national funds through Fundação para a Ciência e Tecnologia. A.P. thanks S. Heilbronner for helpful discussions and critical reading of the manuscript. A.P.'s research is supported by grants from the Deutsche Forschungsgemeinschaft (TRR34, TRR156, SFB766, SFB685, GRK1708 and PE805/5-1), the Deutsches Zentrum für Infektionsforschung (TTU HAARBI) and the European Innovative Medicines Initiative (COMBACTE). S.H. receives financial support from COMBACTE.
J.G. has acted as a consultant for Roche, Nabriva, Paratek and Menarini. J.K. acts as a consultant for Pfizer, 3M and Destiny Pharma. S.M.-K. has received grants from Abbott and Agfa Health. She is receiving research grants from Pfizer and Huvepharma and has a service agreement with AiCuris. A.P. receives a consultant fee from Crucell and research grants from Crucell, Medimmune, MorphoSys and Roche; he has a patent pending for lugdunin. S.H. was a temporary member of the speakers’ bureau for Takeda; has participated in the scientific advisory boards of DNA Electronics, Sandoz, GlaxoSmithKline and Bayer; and has received financial support for research activities from Pfizer and B. Braun. A.S.L. and H.d.L. declare no conflicts of interest.
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Lee, A., de Lencastre, H., Garau, J. et al. Methicillin-resistant Staphylococcus aureus. Nat Rev Dis Primers 4, 18033 (2018). https://doi.org/10.1038/nrdp.2018.33
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