CAM 210

Testing for Mosquito- or Tick-Related Infections

Category:Laboratory   Last Reviewed:November 2018
Department(s):Medical Affairs   Next Review:October 2019
Original Date:February 2019    

Description
Arthropodvectors, including mosquitoes, ticks, fleas, and mites, that feed on vertebrate hosts, can spread bacteria, protozoa, and viruses during feeding to their susceptible host, resulting in a variety of infections and diseases. Arboviruses (Arthropod-borne viruses)include Zika virus, West Nile virus (WNV), chikungunyavirus, denguevirus (DENV), yellow fever virus (YFV), and Colorado tick fever virus (CTF), to name a few. Malaria and babesiosis are both conditions caused by arthropod-borne protozoan parasites, Plasmodium and Babesia, respectively. Conditions caused by arthropod-borne bacteria include rickettsial diseases, ehrlichiosis, anaplasmosis, and Lyme disease, as well as other Borrelia-associated disorders (Calisher, 1994; CDC, 2018). Isolation, identification, and characterization of these various infections depend on the causative agent. Identification methods may include culture testing, microscopy, and staining techniques; moreover, molecular testing, such as nucleic acid amplification testing (NAAT), and serologic testing, including immunofluorescence antibody (IFA) assays and enzyme-linked immunosorbent assays (ELISA), can be used for laboratory diagnosis (Miller et al., 2018).

Background
Hematophagous arthropods, such as mosquitoes, ticks, fleas, and mites, can spread opportunistic bacteria, protozoa, and viruses to host organisms when feeding. Numerous outbreaks of arthropod-borne disease have been documented, including plague, an acute febrile disease caused by Yersinia pestis through the bite of infected fleas, which resulted in more than 50 million deaths in Europe alone during the “Black Death” outbreak. More than 3,000 cases of plague were reported to the World Health Organization (WHO) between 2010 and 2015, with 584 deaths. Today, most cases of plague occur in the Democratic Republic of Congo, Madagascar, and Peru (WHO, 2017). 

The Centers for Disease Control and Prevention (CDC) reported a large increase in the number of vector-borne diseases within the United States and its territories between 2004-2016. More than 640,000 cases were reported during that time; in fact, infections of tick-borne bacteria and protozoa more than doubled during that time frame. “In the United States, 16 vector-borne diseases are reportable to state and territorial health departments, which are encouraged to report them to the National Notifiable Disease Surveillance System (NNDSS). Among the diseases on the list that are caused by indigenous pathogens are Lyme disease (Borrelia burgdorferi); West Nile, dengue and Zika virus diseases; plague (Yersinia pestis); and spotted fever rickettsioses (e.g., Rickettsia rickettsii). Malaria and yellow fever are no longer transmitted in the United States but have the potential to be reintroduced (Rosenberg et al., 2018).” New vector-borne infections are emerging; for example, two unknown, life-threatening RNA viruses spread by ticks have been identified in the U.S. since 2004. Although both tick- and mosquito-borne diseases are increasing across the U.S., the CDC reports that these two vectors are showing different trends. The mosquito-borne diseases are characterized by epidemics; for example, West Nile Virus is essentially limited to the continental U.S. but spread rapidly since its introduction to New York in 1999, whereas chikungunya and dengue primarily occur within the U.S. territories. On the other hand, the tick-borne disease increase occurs in the continental U.S. and has been a gradual, steady rate increase, with Lyme disease comprising 82% of all tick-borne diseases (Rosenberg et al., 2018).

Rickettsial infections 
Rocky Mountain spotted fever (RMSF) is the most common rickettsial infection in the U.S., with 2,553 cases reported to the CDC alone in 2008. RMSF is caused by Rickettsia rickettsia, spread in the U.S. predominantly by Dermacentor variabilis, the American dog tick) and D. andersoni (the Rocky Mountain wood tick), and can be found throughout North America, as well as parts of South America. The Council for State and Territorial Epidemiologists combined RMSF with other rickettsial diseases into the more broad “spotted fever rickettsiosis” designation in 2009. Besides the obligatory tick bite, typical symptoms of RMSF include fever, headache, and rash with the characteristic rash occurring in approximately 90% of patients within five days of illness. If left untreated, RMSF can be fatal but can easily be treated with antimicrobial therapy upon timely diagnosis. Definitive diagnosis of RMSF cannot usually be made via culture because Rickettsia cannot be grown in cell-free culture media, since they are obligate intracellular bacteria requiring living host cells. RMSF diagnosis can be made via either skin biopsy prior to treatment with antibiotics or through serologic testing using indirect immunofluorescence assays (IFAs). IgG antibodies are more specific than IgM antibodies, since the latter can give false-positive results due to cross-reactivity with other bacterial pathogens. A drawback of IFA is that usually it is unreliable for the first five days of infection until antibody levels are high enough for detection. The CDC and major clinical labs do offer a PCR-based assay for RMSF (Sexton & McClain, 2018). 

Since 2001, 13 other human rickettsiae belonging to the spotted fever group (SFG) have been identified. All SFGs can cause fever, headache, and myalgia and are arthropod-borne (primarily ticks and mites). Most patients with an SFG display a rash and/or a localized eschar. Rickettsialpox, caused by R. akari, is transmitted from the bite of a house mouse mite, typically after mouse extermination programs result in a decrease of the mite’s food supply. It is typically a relatively mild disease that can resolve itself without treatment within three weeks, but treatment hastens improvement. Rickettsiosis can also be due to infection with R. parkeri, R. amblyommii, and Rickettsia species 364D (also called R. philipii). Isolation of SFG rickettsiae is rare in clinical practice due to the difficulty of obtaining culture; consequently, serology, immunologic detection from tissue, and PCR are more often used for diagnosis. Microimmunofluorescent (MIF) antibody tests, ELISA, and Western blot immunoassays can be used to detect convalescent IgG and IgM antibodies, but these methods can only be used at least 10-14 days after the onset of illness when antibody concentrations are high enough for detection. PCR is a very specific technique. PCR using tissue samples has higher specificity than whole blood PCR. Immunologic detection from a tissue biopsy requires the use of special laboratory equipment so it is not as frequently used as either the serologic or PCR detection methods (Sexton & McClain, 2017). 

Ehrlichiosis and Anaplasmosis 
Human ehrlichiosis was first reported in 1986, and the causative agent for human granulocytic anaplasmosis, Anaplasma phagocytophilum, was identified in 1994. Both ehrlichiosis and anaplasmosis are transmitted from the bite of infected ticks and have similar clinical and laboratory manifestations. Ehrlichiosis can be caused by Ehrlichia chaffeensis, E. ewingii, and E. muris. Typically, patients have a fever within an incubation period of one to two weeks. Other symptoms can include malaise, myalgia, headache, chills, gastrointestinal distress, and cough. Both leukopenia and thrombocytopenia can occur. Diagnosis via culture is extremely difficult. “Until 1995, only two isolates of E. chaffeensis had been recovered from humans; in both cases, this process required over 30 days of cultivation. The isolation of A. phagocytophilum from three additional patients has been accomplished using a cell culture system derived from human promyelocytic leukemia cells (Sexton & McClain, 2016). IFA testing for bacteria-specific antibodies is the most common method for diagnosing ehrlichiosis and anaplasmosis, but similar to rickettsiae, ELISA, PCR, and immunochemical tissue staining can be used as well. Unlike rickettsiosis, ehrlichiosis and anaplasmosis can also be detected by the presence of characteristic intraleukocytic morulae in a peripheral blood smear or buffy coat smear (Sexton & McClain, 2016). 

Borrelia Infections 
Besides Lyme disease, caused by Borrelia burgdorferi, Borrelia can cause relapsing fever. Tick-borne relapsing fever (TBRF) in North America is primarily caused by B. hermsii, B. turicatae, B. parkeri, B. miyamotoi, and B. mazzottii, and louse-borne relapsing fever (LBRF) is an infection by B. recurrentis (Barbour, 2018; Miller et al., 2018). The characteristic feature of these infections is the relapsing fever due to cyclical spirochetemia caused by antigenic variation of the spirochetes. Each bout of fever lasts 3 to 12 days with temperatures ranged from 39C to 43C. Visual analysis by Giemsa or Wright staining blood smears taken during a febrile episode is common practice. PCR can also be on a variety of samples, including CSF, blood, tissue, or even culture medium. Culture and serologic testing are not typically performed on the Borrelia that cause TBRF and LBRF, due to the lack of facilities that grow these cultures and to cross-reactivity to other antibodies. One exception is using antibodies to the GlpQ protein characteristic of these Borrelia species but not to B. burgdorferi (Lyme disease) (Barbour, 2018).

Protozoa infections 
Babesiosis is due to primarily Babesia microti in the U.S, but B. divergens and B. venatorum are the primary causative agents of babesiosis in Europe and China, respectively. The incubation period of Babesia depends on the mode of transfection: 1-4 weeks following a tick bite or up to 9 weeks following a blood transfusion, even though incubation periods up to six months have been reported. The most common symptoms of infection include a fever, fatigue, malaise, chills, sweats, headache, and myalgia. Immunocompromised individuals can develop relapsing babesiosis due to an absent or impaired production of antibodies, with approximately 20% mortality rate for patients who develop relapsing babesiosis. A majority of patients with babesiosis are also co-infected with other tick-borne bacterial pathogens. “Preferred tools for diagnosis of babesiosis include blood smear for identification of Babesia organisms and polymerase chain reaction (PCR) for detection of Babesia DNA. Serology can be a useful adjunct to blood smear and PCR (Krause & Vannier, 2017).” Serology is not ideal in diagnosing an acute infection, since antibody concentrations remain elevated post-recovery.

Plasmodium falciparum, P. vivax, and P. ovale are responsible for malaria. They are spread by the bite of an Anopheles mosquito, where their sporozoites infect the liver within one to two hours. Within the hepatocyte, they form merozoites. Upon rupturing into the bloodstream, the merozoites infect red blood cells for trophozoite formation, causing the erythrocytic stage of the life cycle, where additional merozoites are released. During this stage of the cycle, the symptoms of malaria, including fever, occur. This process usually takes 12 to 35 days, but clinical manifestations can be delayed in individuals with partial immunity or those who are taking ineffective prophylaxis (Breman, 2018). Other initial symptoms can include irregular heartbeat, cough, anorexia, gastrointestinal distress, sweating, chills, malaise, arthralgia, and myalgia. Malaria, if left untreated, can also include acidosis, hypoglycemia, severe anemia, renal and hepatic impairment, and edema. It can be fatal. Parasite-based diagnosis can include microscopic examination of blood smears, which can often identify the species of Plasmodium, as well as the parasite density, and antigen-based tests. Rapid diagnostic testing (RDT) of the antigens using immunochromatographic methods is available, but the accuracy of the RDT can vary considerably. NAATs can also be used to identify a malarial infection, and NAATs “are typically used as a gold standard in efficacy studies for antimalarial drugs, vaccines, and evaluation of other diagnostic agents” with a “theoretical limit of detection for PCR … estimated at 0.02 to 1 parasite/microL (Hopkins, 2018).”

Viral infections 
Examples of arthropod-borne viruses (arboviruses) include West Nile virus (WNV), dengue, yellow fever virus (YFV), chikungunya, and Colorado tick fever virus, to name a few. In the United States, WNV is the most common arbovirus reported to the CDC. In 2016, 96% of the reported 2,240 cases of domestic arboviruses were WNV, with 61% of the WNV cases reported being neuroinvasive. Neuroinvasive WNV includes meningitis, encephalitis, and acute flaccid paralysis (Burakoff, Lehman, Fischer, Staples, & Lindsey, 2018). In general, most infected individuals are asymptomatic, with only 20-40% of infected patients showing any characteristic symptoms of WNV, including fever, headache, malaise, myalgia, anorexia, and rash. Diagnosis of WNV of a symptomatic individual usually occurs with a WNV IgM antibody capture ELISA (MAC-ELISA) assay. A patient with symptoms of a neurologic infection does require a lumbar puncture. Confirmatory testing can include a plaque reduction neutralization test (PRNT). PCR testing is primarily used with immunocompromised patients who have delayed or absent antibody production, patients with a history of prior flavivirus infections, and blood donors who may be asymptomatic (L. Petersen, 2018). 

Dengue virus (DENV) infection is a result of being bitten by an infected Aedes aegypti or A. albopictus mosquito. Four distinct DENV types of Flavivirus are known: DENV-1, DENV-2, DENV-3, and DENV-4. DENV is endemic throughout many of the tropical regions of the world, but the only region of the U.S. endemic for DENV is Puerto Rico. The last major outbreak occurred in Puerto Rico in 2010, where 26,766 cases of suspected DENV were reported and 47% of all laboratory-tested specimens were positive (CDC, 2013, 2014). “Dengue fever … is an acute febrile illness defined by the presence of fever and two or more of the following, but not meeting the case definition of dengue hemorrhagic fever: headache, retro-orbital or ocular pain, myalgia and/or bone pain, arthralgia, rash, hemorrhagic manifestations … [and] leukopenia. The cardinal feature of dengue hemorrhagic fever is plasma leakage due to increased vascular permeability as evidenced by hemoconcentration (≥20 percent rise in hematocrit above baseline), pleural effusion, or ascites [4]. DHF is also characterized by fever, thrombocytopenia, and hemorrhagic manifestations …. (Thomas, Rothman, Srikiatkhachorn, & Kalayanarooj, 2018).” Laboratory diagnostic testing includes direct detection of viral components in serum or indirect serologic assays. “Detection of viral nucleic acid or viral antigen has high specificity but is more labor intensive and costly; serology has lower specificity but is more accessible and less costly (Thomas et al., 2018).”  Culture testing as a diagnostic tool usually is time-prohibitive. 

Colorado tick fever virus (CTFV) is a Reoviridae transmitted primarily by the Rocky Mountain wood tick (Dermacentor andersoni) in the western U.S. and Canada. Transmission of CTFV has also been reported in blood transfusions. The incubation period can last up to 14 days, and symptoms include fever, headache, chills, myalgia, leukopenia, and prostration. Only 15% of symptomatic patients demonstrate a rash. Serologic tests are usually not helpful until at least 10-14 days for antibody production, whereas RT-PCR can be used on the first day of symptoms (L.R. Petersen, 2017). 

Yellow fever, occurring primarily in sub-Saharan Africa and South America, is a flavivirus spread by mosquitoes that causes hemorrhagic fever with a high fatality rate. An outbreak in Brazil in January-March 2018 resulted in 4 of 10 patients infected with YFV dying. None of those showing symptoms had been vaccinated against YFV. Yellow fever causes hemorrhagic diathesis due to decreased synthesis of vitamin K-dependent coagulation factors, as well as hepatic dysfunction, renal failure, and coagulopathy. Yellow fever diagnosis is typically made by a serologic test using an ELISA-IgM assay; however, this assay does cross-react with other flaviviruses and with the YFV vaccination. Rapid diagnostic testing using either PCR or immunoassay is available. Viral isolation and culture can be performed, but it requires inoculation of mosquitoes or mammalian cell culture. Tissue biopsy, such as liver, cannot be performed on the living patient due to possible fatal hemorrhaging; biopsy would be performed during the post-mortem workup (Monath, 2018). 

Chikungunya virus, endemic in many tropical and subtropical regions of the world, is transmitted by the mosquitoes Aedes aegypti and Aedes albopictus. Within the U.S., chikungunya is prevalent in Puerto Rico, where approximately 25% of blood donors were seropositive; it has also been reported in Florida. Both dengue and Zika are transmitted by the same vectors, so these viruses often co-circulate in a given geographic area. Chikungunya can cause acute febrile polyarthralgia and arthritis. The predominant testing method for diagnosis of chikungunya is the detection of viral RNA via, either RT-PCR or virus serology, using either ELISA or IFA. Viral culture is typically not used as a diagnostic tool but is used for epidemiologic research (Wilson & Lenschow, 2018). 

Types of Testing 

Test

Description

Rationale

Culture

Culture growth depends on the pathogen being studied. If the pathogen is an obligate intracellular organism, then it must be isolated using more sophisticated cell culture techniques. In many circumstances, culture is used for research and/or epidemiology rather than as a diagnostic tool (Biggs et al., 2016; Miller et al., 2018).

At times, culture testing is not as sensitive as either NAAT or serologic testing and can be time-intensive when treatment should not be delayed. Depending on the organism, this may require high biosafety level laboratory for culture growth (Biggs et al., 2016).

Indirect immunofluorescene antibody (IFA) assays

IFA is a serologic assay that can be used to test for the presence of antibodies, such as IgG and IgM, reactive against the pathogen (Biggs et al., 2016).

Depending on the pathogen, IFA can be a useful tool. At times, though, it can cross-react with either a prior vaccination or infection (Monath, 2018). An acute infection can often be determined by  performing IFA in both the acute phase and convalescent phase, where at least a fourfold increase in antibodies is indicative of an acute infection (Biggs et al., 2016). 

Darkfield microscopy 

Darkfield microscopy can be used to detect the presence of microorganisms, such as motile spirochetes (Miller et al., 2018). 

This technique is not widely available, and transport of sample must be done immediately if testing of motile specimen is desired (Miller et al., 2018). 

Blood-smear microscopy 

Blood-smear microscopy can be either thick or thin and is typically performed on a sample stained with an eosin-azure-type dye, such as Giemsa, to look at intracellular structures or morphological features (Biggs et al., 2016). 

This technique should be performed by an experienced microscopist, since it can be inconsistent. As compared to other techniques, this technique is relatively inexpensive (Biggs et al., 2016). 

Nucleic acid amplification testing (NAAT) 

NAATs can include polymerase chain reaction (PCR), real-time PCR (RT-PCR), or other enzyme- dependent amplification testing for the presence of nucleic acids (DNA or RNA). 

NAATs can be specific and sensitive; however, they may not be available at all laboratories and/or can be costly. Some NAATs are available as rapid diagnostic tools. NAATs have been used on serum, whole blood, tissue, CSF, and even formalin-fixed, paraffin-embedded biopsies from autopsy tissues. The sensitivity of the technique can vary depending on the sample; for example, whole blood PCR for R. rickettsii is less sensitive than a similar sample test for E. chaffeensis (Biggs et al., 2016). 

Analytical Validity 
The use of antibodies to detect and diagnose arthropod-associated infections and diseases is a common practice. Johnson et al. in 2000 first reported the use of monoclonal antibody-based capture ELISA testing for a variety of alphaviruses, including chikungunya, flaviviruses, including dengue and yellow fever, and bunyaviruses. They concluded, “IgG ELISA results correlated with those of the standard plaque-reduction neutralization assays. As expected, some test cross-reactivity was encountered within the individual genera, and tests were interpreted within the context of these reactions. The tests were standardized for laboratory diagnosis of arboviral infections, with the intent that they be used in tandem with the corresponding IgM antibody-capture ELISAs (Johnson, Martin, Karabatsos, & Roehrig, 2000).” Kalish and associates also demonstrated that IgG and/or IgM antibody responses can still occur up to 20 years post-infection; consequently, a rise in antibody titer does not necessarily indicate a current, acute infection (Kalish et al., 2001). 

Clinical Validity 
In 2013, Kato and colleagues tested the sensitivity of two different RT-PCR-based assays for Rickettsia — PanR8, an assay that tests for Rickettsia in general, and RRi6, an assay specific for R. rickettsii. Both of these methods were more sensitive in testing for Rickettsia than the nested PCR method of the CDC; moreover, both of these methods are faster than the nested PCR method (1 hr versus 1-2 days, respectively) (Kato et al., 2013). These results were corroborated in 2014 by Denison and colleagues. They used a multiplex PCR assay to correctly identify all cell controls for R. rickettsii, R. parkeri, and R. akari; moreover, no false-positive results were reported using this methodology. “This multiplex real-time PCR demonstrates greater sensitivity than nested PCR assays in FFPE [formalin-fixed, paraffin-embedded] tissues and provides an effective method to specifically identify cases of Rocky Mountain spotted fever, rickettsialpox, and R. parkeri rickettsiosis by using skin biopsy specimens (Denison, Amin, Nicholson, & Paddock, 2014).” 

The FDA has approved the use of the BinaxNOW malaria test for screening and diagnosing malaria. Even though this testing method is considerably faster than other methods (as low as 1.1-1.7 hours complete turnaround time (Ota-Sullivan & Blecker-Shelly, 2013)), the use of BinaxNOW in non-endemic areas is a point of controversy due to relatively low sensitivity (84.2%) and for misclassifying Plasmodium falciparum malaria as non-falciparum (Dimaio, Pereira, George, & Banaei, 2012). Moreover, it has been reported that Salmonella typhi can give a false-positive for malaria using the BinaxNOW test (Meatherall, Preston, & Pillai, 2014).

Regulatory Status 
On 6/29/2017, the FDA approved the Rickettsia Real-Time PCR Assay (K170940) by the Centers for Disease Control and Prevention (CDC) with the following definition: “An in vitro diagnostic test for the detection of Rickettsia spp. nucleic acids in specimens from individuals with signs or symptoms of rickettsial infection and epidemiological risk factors consistent with potential exposure. Test results are used in conjunction with other diagnostic assays and clinical observations to aid in the diagnosis of infection, in accordance with criteria defined by the appropriate public health authorities in the federal government (FDA, 2018).” 

On 9/1/2009, the FDA approved the BinaxNOW Malaria Positive Control Kit (K083744) rapid diagnostic test (RDT), an in vitro qualitative immunochromatographic assay, for use by hospital and commercial laboratories, but it is not approved for individual or physician offices (Arguin & Tan, 2017; FDA, 2018). 

As of 8/7/2018, the FDA has approved the following assays for the detection of West Nile Virus (FDA, 2018): West Nile Virus ELISA IgG model EL0300G and West Nile Virus IgM Capture ELISA model EL0300M by Focus Technologies, Inc., West Nile Virus IgM Capture ELISA model E-WNV02M and West Nile Virus IgG Indirect ELISA by Panbio Limited, West Nile Detect IgM ELISA by Inbios Intl, Inc., Spectral West Nile Virus IgM Status Test by Spectral Diagnostics, Inc., and the EUROIMMUN Anti-West Nile Virus ELISA (IgG) and EUROIMMUN Anti-West Nile Virus ELISA (IgM) by Euroimmun US, Inc. 

Additionally, many labs have developed specific tests that they must validate and perform in house. These laboratory-developed tests (LDTs) are regulated by the Centers for Medicare & Medicaid Services (CMS) as high-complexity tests under the Clinical Laboratory Improvement Amendments of 1988 (CLIA ’88). As an LDT, the U.S. Food and Drug Administration has not approved or cleared this test; however, FDA clearance or approval is not currently required for clinical use. 

Policy 
Application of coverage criteria is dependent upon an individual’s benefit coverage at the time of the request.

  1. Concerning suspected cases of rickettsial diseases (see signs and symptoms below), including Rocky Mountain spotted fever, Rickettsia parkeri rickettsiosis, Rickettsia species 364D rickettsiosis, Rickettsia spp (mild spotted fever), and R. akari (rickettsialpox):
    1. The following is considered MEDICALLY NECESSARY:
      • Indirect immunofluorescence antibody (IFA) assay for IgG antibodies
      • A limit of one unit of IFA assay meets coverage criteria.
    2. The following is considered NOT MEDICALLY NECESSARY:
      • Standard blood culture; OR
      • Nucleic acid amplification testing (NAAT), including PCR; OR
      • IFA assay for IgM antibodies;
      • More than one unit of IFA testing
    3. Typical signs and symptoms of rickettsial diseases usually begin 3 – 12 days after initial bite and can include (Biggs et al., 2016):
      • Fever
      • Headache
      • Chills
      • Malaise
      • Myalgia
      • Nausea
      • Vomiting
      • Abdominal pain
      • Photophobia
      • Anorexia
      • Skin rash
      • Ulcerative lesion with regional lymphadenopathy (for Rickettsia species 364D rickettsiosis)
  2. Concerning suspected cases of ehrlichiosis and/or anaplasmosis (see signs and symptoms below):
    1. The following is considered MEDICALLY NECESSARY:
      • NAAT, including PCR, of whole blood; AND
      • Indirect immunofluorescence antibody (IFA) assay for IgG antibodies; AND
      • Microscopy for morulae detection
    2. The following is considered NOT MEDICALLY NECESSARY:
      • IFA assay for IgM antibodies; OR
      • Standard blood culture
    3. Typical signs and symptoms of ehrlichiosis and/or anaplasmosis usually begin 5-14 days after an infected tick bite, and they include (Biggs et al., 2016):
      • Fever
      • Headache
      • Malaise
      • Myalgia
      • Shaking chills
      • Gastrointestinal issues, including nausea, vomiting, and diarrhea, in ehrlichiosis
  3. Concerning suspected cases of tick-borne relapsing fever (TBRF) caused by Borrelia  hermsii, B. parkerii, B. mazzottii, or B. turicatae (see signs and symptoms below):
    1. The following is considered MEDICALLY NECESSARY:
      • Dark-field microscopy of peripheral blood smear; OR
      • Microscopy of Wright- or Giemsa-stained blood smear
    2. The following is considered NOT MEDICALLY NECESSARY:
      • IFA assay for either IgG or IgM for Borrelia; OR
      • Culture testing for Borrelia
    3. The following is considered to be INVESTIGATIONAL:
      • NAAT, including PCR
    4. Typical signs and symptoms include (CDC, 2015c):
      • Recurring febrile episodes that last approximately 3 days separated by approximately 7 days
    5. Nonspecific symptoms that occur in at least 50% of cases include headache, myalgia, chills, nausea, arthralgia, and vomiting
  4. Concerning suspected cases of babesiosis (see signs and symptoms below):
    1. The following is considered MEDICALLY NECESSARY:
      • Giemsa- or Wright-stain of blood smear
    2. The following is considered NOT MEDICALLY NECESSARY:
      • IFA assay for either Babesia IgG or IgM; OR
      • NAAT, including PCR
    3. Typical signs and symptoms of babesiosis can include (CDC, 2012):
      • Hemolytic anemia
      • Splenomegaly
      • Hepatomegaly
      • Jaundice
      • Nonspecific flu-like symptoms such as fever, chills, body aches, weakness, and fatigue 
  5. Concerning suspected cases of malaria (see signs and symptoms below):
    1. The following is considered MEDICALLY NECESSARY:
      • Smear microscopy to diagnose malaria, determine the species of Plasmodium, identify the parasitic life-cycle stage, and/or quantify the parasitemia
        • Can be repeated up to three times within three days if initial microscopy is negative in suspected cases of malaria; OR
      • Rapid immunochromatographic diagnostic test
    2. The following is considered NOT MEDICALLY NECESSARY:
      • NAAT, including PCR
      • IFA for Plasmodium antibodies
    3. Typical signs and symptoms of malaria can include (Arguin & Tan, 2017):
      • Fever
      • Influenza-like symptoms such as chills, headache, body aches, and so on
      • Anemia
      • Jaundice
      • Seizures
      • Mental confusion
      • Kidney failure
      • Acute respiratory distress syndrome
  6. Concerning suspected cases of chikungunya virus (see signs and symptoms below):
    1. The following is considered MEDICALLY NECESSARY:
      • Viral culture for diagnosis; OR
      • NAAT, including PCR, for presence of chikungunya in serum sample; OR
      • Indirect immunofluorescence antibody (IFA) assay for IgM antibodies during both the acute and convalescent phase
    2. Typical signs and symptoms of chikungunya include (Staples et al., 2017):
      • High fever (>102◦F or 39◦C)
      • Joint pains (usually multiple joints, bilateral, and symmetric)
      • Headache
      • Myalgia
      • Arthritis
      • Conjunctivitis
      • Nausea
      • Vomiting
      • Maculopapular rash
  7. Concerning suspected cases of West Nile Virus (WNV) (see signs and symptoms below):
    1. The following is considered MEDICALLY NECESSARY:
      • IFA for WNV-specific IgM or IgG antibodies in either serum or CSF; AND
      • Plaque reduction neutralization test for WNV
    2. The following is considered NOT MEDICALLY NECESSARY:
      • NAAT, including PCR, for WNV
    3. Typical signs and symptoms of WNV include (Nasci et al., 2013):
      • Headache
      • Myalgia
      • Arthralgia
      • Gastrointestinal symptoms
      • Maculopapular rash
      • Less than 1% develop neuroinvasive WNV with symptoms of meningitis, encephalitis, or acute flaccid paralysis
  8. Concerning suspected cases of Yellow Fever Virus (YFV) (see signs and symptoms below):
    1. The following is considered MEDICALLY NECESSARY:
      • Plaque reduction neutralization test for YFV; AND
      • NAAT, including PCR, for YFV; AND
      • Serologic assays to detect virus-specific IgM and IgG antibodies
    2. Typical signs and symptoms of yellow fever include (Gershman & Staples, 2017):
      • Nonspecific influenzalike syndrome, including fever, chills, headache, backache, myalgia, prostration, nausea, and vomiting in initial illness
      • Toxic form of disease symptoms include jaundice, hemorrhagic symptoms, and multisystem organ failure
  9. Concerning suspected cases of Dengue virus (DENV) (see signs and symptoms below):
    1. The following is considered MEDICALLY NECESSARY:
      • Plaque reduction neutralization test for DENV; AND
      • NAAT, including PCR, for DENV; OR
      • IgM antibody capture ELISA (MAC-ELISA); OR
      • NS1 ELISA
    2. The following is considered NOT MEDICALLY NECESSARY:
      • IgG-ELISA
      • Hemagglutination testing
    3. Typical signs and symptoms of dengue can include (CDC, 2014):
      • Fever
      • Headache
      • Retro-orbital eye pain
      • Myalgia
      • Arthralgia
      • Erythematous maculopapular rash
      • Petechiae
      • Leukopenia
  10. Concerning suspected cases of Colorado Tick Fever (CTF) (see signs and symptoms below):
    1. The following is considered MEDICALLY NECESSARY:
      • Virus-specific IFA-stained blood smears; OR
      • IFA for CTF-specific antibodies
    2. Typical signs and symptoms of CTF can include (CDC, 2015a):
      • Fever
      • Chills
      • Headache
      • Myalgia
      • Malaise
      • Sore throat
      • Vomiting
      • Abdominal Pain
      • Maculopapular or petechial rash

Rationale
Centers for Disease Control and Prevention (CDC) 
Diagnosis and Management of Tickborne Rickettsial Diseases (Biggs et al., 2016): In 2016, the CDC released its guidelines and recommendations concerning Rickettsial diseases, including Rocky Mountain spotted fever, in the MMWR. The table below summarizes its recommended diagnostic tests for tick-borne rickettsial diseases:

Table 4. Recommended Diagnostic Tests for Tickborne Rickettsial Diseases 

PCR
Disease Whole blood Eschar biopsy or swab Rash biopsy Microscopy for morulae detection IFA assay for IgG antibodies (acute and convalescent)*
Rocky Mountain spotted fever Yes+   Yes   Yes
Rickettsia parkeri rickettsiosis   Yes Yes   Yes
Rickettsia species 364D rickettsiosis   Yes     Yes
Ehrichia chaffeensis enrlichiosis (human monocytic ehrlichiosis Yes     Yes Yes
Ehrlichia ewingil ehrlichiosis Yes     Yes Yes
Ehlichia murls-like agent ehrlichiosis Yes       Yes
Human anaplasmosis (human granulocytic anaplasmosis) Yes     Yes Yes

Abbreviations: IFA = indirect immunofluorescence antibody; IgG = immunoglobulin G; PCR = polymerase chain reaction.
*IFA assay is insensitive during the first week of illness for most tick-borne rickettsial diseases; a sample should be collected during this interval (acute specimen), and a second sample should be collected 2-4 weeks later (convalescent specimen) for comparison. Elevated titers alone are not sufficient to diagnose infection with tickborne rickettsial diseases; serial titers are needed for confirmation. Demonstration of at least a fourfold rise in antibody titer is considered confirmatory evidence of acute infection.
+ PCR of whole blood samples for Rickettsia rickettsii has low sensitivity; sensitivity increases in patients with severe disease. 

To summarize the recommendations, even though indirect immunofluorescence antibody assays (IFAs) are insensitive typically during the first week of an acute infection, they are the standard reference for tickborne rickettsial infections and that a minimum of two tests are to be performed for diagnosis. Usually, one sample is taken early, after the initial symptoms are present, and a second sample is taken 2-4 weeks later. A minimum of a fourfold rise in antibody titer is required to confirm diagnosis. In cases of ehrlichiosis and anaplasmosis, during the first week, PCR amplification can be used on whole blood for diagnosis, but PCR has low sensitivity in Rocky Mountain spotted fever, except in patients with severe disease. Morulae detection via either blood-smear or buffy-coat preparation microscopy can also be indicative of ehrlichiosis or anaplasmosis. "Rickettsiae cannot be isolated with standard blood culture techniques because they are obligate intracellular pathogens; specialized cell culture methods are required. Because of limitations in availability and facilities, culture is not often used as a routine confirmatory diagnostic method for tickborne rickettsial diseases (Biggs et al., 2016)."

Tickborne relapsing fever (TBRF) (CDC, 2015c): In the U.S., TBRF can be caused by Borrelia hermsii, B. parkerii, and B. turicatae, with B. hermsii being the most common causative agent. Due to the relapsing nature of TBRF (usually ~3 days per febrile episode followed by an afebrile period of approximately one week), the CDC recommends testing during a febrile episode, since spirochetemia is at its highest (100-1,000 times higher than even early cases of Lyme disease). "The definitive diagnosis of TBRF may be based on the observation of relapsing fever spirochetes (Borrelia hermsii, B. turicatae, or B. parkerii in the U.S.) in peripheral blood smears of a symptomatic person by a microscopist trained in spirochete identification. Although best visualized by dark field microscopy, the organisms can also be detected using Wright-Giemsa or acridine orange stains. … Although not valuable for making an immediate diagnosis, serologic testing is available through public health laboratories and some private laboratories. Acute serum should be taken within 7 days of symptom onset and convalescent serum should be taken at least 21 days after symptoms start. Early antibiotic treatment may blunt the antibody response and the antibody levels may wane quickly during the months after exposure. To confirm the diagnosis of TBRF, Borrelia-specific antibody titers should increase 4-fold between acute and convalescent serum samples, and convalescent serum antibody levels should be at least two standard deviations above pooled negative controls. Serologic testing for TBRF is not standardized and results may vary by laboratory. Patients with TBRF may have false-positive tests for Lyme disease because of the similarity of proteins between the two organisms. Incidental laboratory findings include normal to increased white blood cell count with a left shift towards immature cells, a mildly increased serum bilirubin level, mild to moderate thrombocytopenia, elevated erythrocyte sedimentation rate (ESR), and slightly prolonged prothrombin time (PT) and partial thromboplastin time (PTT) (CDC, 2015c)."

Colorado Tick Fever (CTF) (CDC, 2015b): As of 2015, CTF was reportable in Arizona, Colorado, Montana, Oregon, Utah, and Wyoming. "Laboratory diagnosis of CTF is generally accomplished by testing of serum to detect viral RNA or virus-specific immunoglobulin (Ig) M and neutralizing antibodies. Antibody production can be delayed with CTF, so tests that measure antibodies may not be positive for 14–21 days after the onset of symptoms. RT-PCR (reverse-transcriptase polymerase chain reaction) is a more sensitive test early in the course of disease. CTF testing is available at some commercial and state health department laboratories and at CDC. Contact your state or local health department for assistance with diagnostic testing. They can help you determine if samples should be sent to the CDC Arbovirus Diagnostic Laboratory for further testing (CDC, 2015b)."

Babesiosis (CDC, 2012): According to the CDC website, the most recent update about babesiosis for health professionals is from 2012 (with revision in 2013). Diagnosis can be challenging due to the nonspecific clinical manifestations of the disease. "For acutely ill patients, the findings on routine laboratory testing frequently include hemolytic anemia and thrombocytopenia. Additional findings may include proteinuria, hemoglobinuria, and elevated levels of liver enzymes, blood urea nitrogen, and creatinine. If the diagnosis of babesiosis is being considered, manual (non-automated) review of blood smears should be requested explicitly. In symptomatic patients with acute infection, Babesia parasites typically can be detected by light-microscopic examination of blood smears, although multiple smears may need to be examined. Sometimes it can be difficult to distinguish between Babesia and Plasmodium (especially P. falciparum) parasites and even between parasites and artifacts (such as stain or platelet debris). Consider having a reference laboratory confirm the diagnosis — by blood-smear examination and, if indicated, by other means, such as molecular and/or serologic methods tailored to the setting/species (CDC, 2012)."

Malaria (Arguin & Tan, 2017): The CDC considers smear microscopy as the gold standard in diagnosing malaria, since it can determine the species, identify the stage of parasitic life-cycle, and quantify the parasitemia; however, microscopy should be performed within a few hours due to the timeliness of diagnosis and treatment of disease. "It is an unacceptable practice to send these tests to an offsite laboratory or batch them for results to be provided days later." In the event that microscopy is unavailable, rapid immunochromatographic diagnostic tests (RDTs) that typically use a dipstick or cassette can be used, but RDTs cannot usually distinguish between the different pathogenic species and are less sensitive than either microscopy or PCR. "In addition, CDC recommends that positive and negative RDT results always be confirmed by microscopy in U.S. health care settings… PCR tests are also available for detecting malaria parasites. Although these tests are more sensitive than routine microscopy, results are not usually available as quickly as microscopy results should be, thus limiting the utility of this test for acute diagnosis. PCR testing is most useful for definitively identifying the species of malaria parasite and detecting mixed infections. Species confirmation by PCR is available at the CDC malaria laboratory (Arguin & Tan, 2017)."

Chikungunya (Staples, Hills, & Powers, 2017): In the CDC Yellow Book, concerning the chikungunya virus, they recommend that "the differential diagnosis of chikungunya virus infection depends on the clinical signs and symptoms, as well as where the person was suspected of being infected." The other diseases to consider include: Zika, malaria, leptospirosis, parvovirus, group A Streptococcus, rubella, measles, dengue, enterovirus, adenovirus, alphavirus infections, post-infectious arthritis, and rheumatic conditions. Laboratory diagnosis is done by serum testing for detection of virus, viral nucleic acids, or virus-specific IgM and neutralizing antibodies. "During the first week after onset of symptoms, chikungunya can often be diagnosed by performing viral culture or nucleic acid amplification on serum. Virus-specific IgM and neutralizing antibodies normally develop toward the end of the first week of illness. Therefore, to definitively rule out the diagnosis, convalescent-phase samples should be obtained from patients whose acute-phase samples test negative. Testing for chikungunya virus is performed at CDC, several state health department laboratories, and several commercial laboratories (Staples et al., 2017)."

West Nile Virus (WNV) (Nasci et al., 2013): "WNV infections are most frequently confirmed by detection of anti-WNV immunoglobulin (Ig) M antibodies in serum or cerebrospinal fluid (CSF). The presence of anti-WNV IgM is usually good evidence of recent WNV infection, but may indicate infection with another closely related flavivirus (e.g., St. Louis encephalitis). Because anti-WNV IgM can persist in some patients for >1 year, a positive test result occasionally may reflect past infection unrelated to current disease manifestations. Serum collected within 8 days of illness onset may lack detectable IgM, and the test should be repeated on a convalescent-phase sample. IgG antibody generally is detectable shortly after the appearance of IgM and persists for years. Plaque-reduction neutralization tests (PRNT) can be performed to measure specific virus-neutralizing antibodies. A fourfold or greater rise in neutralizing antibody titer between acute- and convalescent-phase serum specimens collected 2 to 3 weeks apart may be used to confirm recent WNV infection and to discriminate between cross-reacting antibodies from closely related flaviviruses." NAAT may not be suitable in most cases since the concentrations of WNV RNA are so low by the time a patient begins to show symptoms of infection; however, NAAT may be suitable in immunocompromised individuals who have either delayed or absent antibody development.

Yellow Fever Virus (YFV) (Gershman & Staples, 2017): Isolation of the virus or NAAT should be performed as early as possible in suspected cases of YFV. "However, by the time more overt symptoms are recognized, the virus or viral RNA might be undetectable. Therefore, virus isolation and nucleic acid amplification should not be used to rule out a diagnosis of yellow fever … Serologic assays to detect virus-specific IgM and IgG antibodies (sic). Because of cross-reactivity between antibodies raised against other flaviviruses, more specific antibody testing, such as a plaque reduction neutralization test, should be done to confirm the infection (Gershman & Staples, 2017)." Since YFV is a nationally notifiable disease, clinicians should contact their state and/or local health departments according to their respective local, state, and/or federal guidelines.

Dengue (CDC, 2017): Diagnosis of dengue can be via isolation of virus, serological tests such as immunoassays, and molecular methods, including RT-PCR. The CDC’s testing algorithm for dengue is as follows:

  1. PCR — PCR of serum sample within first 5 days of symptom can detect DENV usually with 80-90% sensitivity; however, a negative test result in the first five days should be corroborated by serological testing after the 5th day of illness.
  2. MAC-ELISA (IgM antibody capture ELISA) — even though this testing is limited due to cross reactivity with other flaviviruses, it is “the most commonly employed in diagnostic laboratories” and is commercially available.
  3. IgG-ELISA — this method can be used to determine past dengue infection or used to monitor rise in titer between the acute and convalescent phases of a dengue infection. The two tests should be performed at least seven days apart.
  4. NS1 ELISA — The non-structural protein 1 (NS1) of dengue can be used to diagnose an acute infection between 1 and 18 days post onset of symptoms. “The NS1 assay may also be useful for differential diagnostics between flaviviruses because of the specificity of the assay.”
  5. PRNT (Plaque Reduction and Neutralization Test) — PRNT can be used as a serological specificity tool in convalescent sera by measuring the titer of the neutralizing antibodies to determine the level of protective antibodies. “The assay is a biological assay based on the principle of interaction of virus and antibody resulting in inactivation of virus such that it is no longer able to infect and replicate in cell culture. Some of the variability of this assay is differences in interpretation of the results because of the cell lines and virus seeds used, as well as the dilution of the sera.” A high throughput version of the PRNT that utilizes a colorimetric assay is called microneutralization PRNT.

2018 Infectious Diseases Society of America (IDSA) and the American Society for Microbiology (ASM) (Miller et al., 2018) 
Laboratory Diagnosis of Tickborne Infections: The information given below outlines the diagnostic procedures for tickborne infections and is taken from Table 47 of the 2018 IDSA/ASM guidelines. 

Bacteria

Etiologic Agents

Diagnostic Procedures

Optimum Specimens

Relapsing fever borreliae
Borrelia hermsii (western U.S.)
Borrelia parkeri (western U.S.)
Borrelia turicatae (southwestern U.S.)
Borrelia mazzottii (southern U.S.)

Primary test: Darkfield microscopy or Wright, Giemsa, or Diff-Quik stains of peripheral thin or/ and thick blood smears. Can be seen in direct wet preparation of blood in some cases.

Other testing: NAAT, Culture, Serologic testing

Blood or bone marrow for the primary test. Blood or body fluids for NAAT. Serum for culture or serologic testing.

Borrelia miyamotoi (B. miyamotoi infection, hard tick-borne relapsing fever)

Primary test: NAAT

Serology: EIA for detection of antibodies to recombinant GlpQ antigen

Blood for NAAT and serum for serology.

Anaplasma phagocytophilum (human granulocytotropic anaplasmosis)

Primary test: NAAT

Alternate Primary (if NAAT is unavailable): Wright or Giemsa stain of peripheral blood or buffy coat leukocytes during week first week of infection.

Serology: Acute and convalescent IFA titers for IgG-class antibodies to A. phagocytophilum antibodies

Immunohistochemical staining of Anaplasma antigens in formalin-fixed, paraffin-embedded specimens

Blood for both NAAT and Wright or Giemsa stain

 

Serum for Serology

 

Bone marrow biopsies or autopsy tissues (spleen, lymph nodes, liver, and lung) for IHC staining

Ehrlichia chaffeensis (human monocytotropic ehrlichiosis)
Ehrlichia muris
Ehrlichia ewingii 

Primary test: NAAT (Only definitive diagnostic assay for E. ewingii)

Wright or Giemsa stain of peripheral blood or buffy coat leukocytes smear during first week of infection

Serology: acute and convalescent IFA titers for Ehrlichia IgG-class antibodies

Immunohistochemical staining of Ehrlichia antigens in formalin-fixed, paraffin-embedded specimens 

Whole blood for NAAT

Blood for Wright or Giemsa stain

 

Serum for serology

Bone marrow biopsies or autopsy tissues (spleen, lymph nodes, liver and lung) for IHC staining 

Rickettsia rickettsii (RMSF)
Other spotted fever group Rickettsia spp (mild spotted fever)
R. typhi (murine typhus)
R. akari (rickettsialpox)
R. prowazekii (epidemic typhus)

Serology: acute and convalescent IFA for Rickettsia sp IgM and IgG antibodies

NAAT

Immunohistochemical staining of spotted fever group rickettsiae antigens (up to first 24 h after antibiotic therapy initiated) in formalin-fixed, paraffin-embedded specimens

Serum for serology

Skin biopsy (preferably a maculopapule containing petechiae or the margin of an eschar) or autopsy tissues (liver, spleen, lung, heart, and brain) for NAAT

Skin biopsy (preferably a maculopapule containing petechiae or the margin of an eschar) or autopsy tissues (liver, spleen, lung, heart, and brain) for IHC staining 

Protozoa

Etiologic Agents Diagnostic Procedures Optimum Specimens

Babesia microti
Babesia spp

Primary test: Giemsa, Wright, Wright-Giemsa stains of peripheral thin and thick  Whole blood (EDTA vacutainer tube is a second choice) for staining  

The IDSA/ASM does note that most PCR-based assays for babesiosis only detect B. microti, even though there are at least three other species of Babesia that can cause the infection. "Real time PCR available from CDC and reference labs… Serology does not distinguish between acute and past infection (Miller et al., 2018)."

Their recommendation for the main diagnostic testing for malaria due to Plasmodium falciparum, P. ovale, P. vivax, P. malariae, and P. knowlesi is "Stat microscopic examination of Giemsa-stained thick and thin blood films (repeat testing every 12–24 h for a total of 3 exams before ruling out malaria); rapid antigen detection tests followed by confirmatory blood films within 12–24 h." They make the following special remark: "Antigen tests lack sensitivity with low parasitemia and non-falciparum malaria and do not differentiate all species. PCR from some reference laboratories will detect and differentiate all species. Calculation of percentage parasitemia (using thick or thin blood films) is required for determining patient management and following response to therapy (Miller et al., 2018)." Concerning dengue virus DENV, "Plaque reduction neutralization tests (PRNTs) are considered the reference standard for detection of antibodies to arthropod-borne viruses (arboviruses) and provide improved specificity over commercial serologic assays; however, due to the complexity of testing, PRNT is currently only available at select public health laboratories and the CDC." They note that false-positives for antibodies to DENV may not necessarily indicate DENV infection, since it can also be indicative of a prior flavivirus infection, such as West Nile virus or Zika virus. They do state the following concerning the use of NAAT, "Detection of DENV RNA by NAAT is preferred for acutely ill patients. Recently, detection of the DENV NS1 antigen, which is secreted from infected host cells as early as 1 day after symptom onset and up to 10 days thereafter, has become an acceptable alternative to NAAT for diagnosis of acute DENV infection (Miller et al., 2018)."

For West Nile Virus (WNV), they state: "Laboratory diagnosis of WNV, and most other arboviruses, is typically accomplished by detecting virus-specific IgM- and/or IgG-class antibodies in serum and/or CSF." Possible false-positives can occur if a patient has been vaccinated against yellow fever or if they have had a previous infection of another flavivirus. They do note that WNV RNA detection via NAAT can be performed on either the serum or CSF for immunosuppressed patients.  

American Academy of Pediatrics 2018 Redbook 
Babesiosis (AAP, 2018a): "Acute, symptomatic cases of babesiosis typically are diagnosed by microscopic identification of Babesia parasites on Giemsa- or Wright-stained blood smears… PCR assay is particularly recommended for use in early infection, when parasites are more difficult to visualize on blood smear. However, PCR assay should be used with caution when monitoring response to therapy, because B. microti can be detected for weeks and months after parasites no longer are visualized on blood smear." They do state that antibody testing can be useful in distinguishing between Babesia and Plasmodium infections whenever blood smear examinations and travel histories are inconclusive or for detecting individuals with very low levels of parasitemia.

Non-Lyme Borrelia Infections (AAP, 2018b): Dark-field microscopy and Wright-, Giemsa-, or acridine orange-stained preparations of blood smears can be used to observe the presence of spirochetes in the initial febrile episode, but their presence is more difficult to determine in future recurrences. Both enzyme immunoassay and Western immunoblot analysis can detect serum antibodies; however, "these antibody tests are not standardized and are affected by antigenic variations among and within Borrelia species and strains." As of publication, PCR and antibody-based testing were still under development and were not widely available.

Ehrlichia, Anaplasma, and Related Infections (AAP, 2018e): PCR testing should be performed within the first week of illness to diagnose anaplasmosis, ehrlichiosis, and other Anaplasmataceae infections because doxycycline treatment rapidly decreases the sensitivity of PCR. Consequently, negative PCR results do not necessarily indicate a lack of infection. Occasionally, Giemsa- or Wright staining of blood smears can be performed to identify the presence of the morulae of Anaplasma in the first week of illness. Culture testing for isolation is not performed. "Immunoglobulin (Ig) M serologic assays are prone to false-positive reactions, and IgM … can remain elevated for lengthy periods of time, reducing its diagnostic utility. Serologic testing may be used to demonstrate a fourfold change in IgG-specific antibody titer by indirect immunofluorescence antibody (IFA) assay between paired acute and convalescent specimens taken 2 to 4 weeks apart."

Rocky Mountain Spotted Fever (RMSF) (AAP, 2018h): "The gold standard for serologic diagnosis of RMSF is the indirect immunofluorescence antibody (IFA) test. A negative serologic test result from the acute phase does not rule out a diagnosis of RMSF in any case… A fourfold or greater increase in antigen-specific IgG between acute and convalescent sera obtained 2 to 4 weeks apart confirms the diagnosis (6 weeks for convalescent serum for Rickettsia africae)."

Rickettsialpox (AAP, 2018g): Rickettsialpox can be mistaken for other rickettsial infections. Ideally, the use of R. akari-specific antigen is recommended for serologic diagnosis, but it has limited availability. Otherwise, indirect IFA for R. rickettsia, the causative agent of RMSF, since R. akari has extensive cross-reactivity. Again, a demonstration of at least a fourfold increase in antibody titers taken 2-6 weeks apart is indicative of infection.

Chikungunya (AAP, 2018c): "Laboratory diagnosis generally is accompanied by testing serum to detect virus, viral nucleic acid, or virus-specific immunoglobulin (Ig) M and neutralizing antibodies." RT-PCR can be used to diagnose chikungunya during the first week after onset of symptoms since chikungunya-specific antibodies have not formed at that time. After the first week, serum testing of IgM or a plaque-reduction neutralization test can be performed.

Dengue (AAP, 2018d): "Dengue virus is detectable by RT-PCR or NS1 antigen EIAs from the beginning of the febrile phase until day 7 to 10 after illness onset." Cross-reactivity occurs between anti-dengue virus IgM and other flaviviruses, including Zika. IgG EIA and hemagglutination testing is not specific for diagnosis of dengue, and IgG antibodies remain elevated for life; consequently, a fourfold increase in IgG between the acute and convalescent phase can confirm recent infection. "Reference testing is available from the Dengue Branch of the Centers for Disease Control and Prevention."

Malaria (AAP, 2018f): Microscopic identification of Plasmodium on both thick and thin blood films should be performed. "If initial blood smears test negative for Plasmodium species but malaria remains a possibility, the smear should be repeated every 12 to 24 hours during a 72-hour period… Serologic testing generally is not helpful, except in epidemiologic surveys… Species confirmation and antimalarial drug resistance testing are available free of charge at the Centers for Disease Control and Prevention (CDC) for all cases of malaria diagnosed in the United States." One FDA-approved RADT is available in the U.S. to hospitals and commercial labs; however, both positive and negative test results must be corroborated by microscopic examination.

West Nile Virus (WNV) (AAP, 2018i): PCR is not recommended for diagnosis of WNV in immunocompetent patients since WNV RNA is usually no longer detectable by the initial onset of symptoms. "Detection of anti-WNV immunoglobulin (Ig) M antibodies in serum or CSF is the most common way to diagnose WNV infection." Anti-WNV IgM levels can remain elevated for longer than 1 year, so a positive test result may be indicative of a prior infection. "Plaque-reduction neutralization tests can be performed to measure virus-specific neutralizing antibodies and to discriminate between cross-reacting antibodies from closely related flaviviruses. A fourfold or greater increase in virus-specific neutralizing antibodies between acute-and convalescent-phase serum specimens collected 2 or 3 weeks apart may be used to confirm recent WNV infection."

International Encephalitis Consortium (IEC) (Venkatesan et al., 2013)
In 2013, the IEC released their Case Definitions, Diagnostic Algorithms, and Priorities in Encephalitis. Concerning arboviruses, they state the following: "For most arboviruses, serologic testing of serum and CSF is preferred to molecular testing, since the peak of viremia typically occurs prior to symptom onset. For example, in patients with West Nile virus (WNV) associated with neuroinvasive disease, CSF PCR is relatively insensitive (57%) compared with detection of WNV IgM in CSF. The cumulative percentage of seropositive patients increases by approximately 10% per day during the first week of illness, suggesting the need for repeat testing if the suspicion for disease is strong in those with initially negative results. Notably, arbovirus IgM antibodies may be persistently detectable in the serum and, less commonly, in the CSF, for many months after acute infection, and therefore may not be indicative of a current infection. Therefore, if possible, documentation of acute infection by seroconversion and/or 4-fold or greater rises in titre using paired sera is recommended (Venkatesan et al., 2013)."

References 

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  32. Miller, J. M., Binnicker, M. J., Campbell, S., Carroll, K. C., Chapin, K. C., Gilligan, P. H., . . . Yao, J. D. (2018). A Guide to Utilization of the Microbiology Laboratory for Diagnosis of Infectious Diseases: 2018 Update by the Infectious Diseases Society of America and the American Society for Microbiologya. Clinical Infectious Diseases, ciy381- ciy381. doi:10.1093/cid/ciy381
  33. Monath, T. P. (2018, 03/30/2018). Yellow Fever. UpToDate. Retrieved from https://www.uptodate.com/contents/yellow-fever
  34. Nasci, R., Fischer, M., Lindsey, N., Lanciotti, R., Savage, H., Komar, N., . . . Petersen, L. (2013). West Nile Virus in the United States: Guidelines for Surveillance, Prevention, and Control. Ft. Collins, CO: CDC Retrieved from https://www.cdc.gov/westnile/resources/pdfs/wnvguidelines.pdf.
  35. Ota-Sullivan, K., & Blecker-Shelly, D. L. (2013). Use of the rapid BinaxNOW malaria test in a 24-hour laboratory associated with accurate detection and decreased malaria testing turnaround times in a pediatric setting where malaria is not endemic. J Clin Microbiol, 51(5), 1567-1569. doi:10.1128/jcm.00293-13
  36. Petersen, L. (2018, 07/30/2018). Clinical manifestations and diagnosis of West Nile virus infection. UpToDate. Retrieved from  https://www.uptodate.com/contents/clinical-manifestations-and-diagnosis-of-west-nile-virus-infection
  37. Petersen, L. R. (2017, 08/14/2014). Arthropod-borne encephalitides. UpToDate. Retrieved from https://www.uptodate.com/contents/arthropod-borne-encephalitides
  38. Rosenberg, R., Lindsey, N. P., Fischer, M., Gregory, C. J., Hinckley, A. F., Mead, P. S., . . . Petersen, L. R. (2018). Vital Signs: Trends in Reported Vectorborne Disease Cases - United States and Territories, 2004-2016. MMWR Morb Mortal Wkly Rep, 67(17), 496-501. doi:10.15585/mmwr.mm6717e1
  39. Sexton, D. J., & McClain, M. T. (2016, 08/15/2016). Human ehrlichiosis and anaplasmosis. UpToDate. Retrieved from https://www.uptodate.com/contents/human-ehrlichiosis-and-anaplasmosis
  40. Sexton, D. J., & McClain, M. T. (2017, 09/12/2018). Other spotted fever group rickettsial infections. UpToDate. Retrieved from https://www.uptodate.com/contents/other-spotted-fever-group-rickettsial-infections 
  41. Sexton, D. J., & McClain, M. T. (2018, 05/29/2018). Clinical manifestations and diagnosis of Rocky Mountain spotted fever. UpToDate. Retrieved from https://www.uptodate.com/contents/clinical-manifestations-and-diagnosis-of-rocky-mountain-spotted-fever
  42. Staples, J., Hills, S., & Powers, A. (2017). Chapter 3 Infectious Diseases Related to Travel: Chikungunya. In G. Brunette (Ed.),
  43. CDC Yellow Book 2018: Health Information for International Travel. New York: Oxford University Press.
  44. Thomas, S., Rothman, A., Srikiatkhachorn, A., & Kalayanarooj, S. (2018, 07/24/2018). Dengue virus infection: Clinical manifestations and diagnosis. UpToDate. Retrieved from https://www.uptodate.com/contents/dengue-virus-infection-clinical-manifestations-and-diagnosis
  45. Venkatesan, A., Tunkel, A. R., Bloch, K. C., Lauring, A. S., Sejvar, J., Bitnun, A., . . . International Encephalitis, C. (2013). Case definitions, diagnostic algorithms, and priorities in encephalitis: consensus statement of the international encephalitis consortium. Clin Infect Dis, 57(8), 1114-1128. doi:10.1093/cid/cit458
  46. WHO. (2017, 10/31/2017). Plague. News-Room. Retrieved from http://www.who.int/news-room/fact-sheets/detail/plague
  47. Wilson, M. E., & Lenschow, D. J. (2018, 05/07/2018). Chikungunya fever. UpToDate. Retrieved from https://www.uptodate.com/contents/chikungunya-fever 

Coding Section 

 Code

Number 

Description 

CPT 

86757

Antibody; Rickettsia; Immunoassay Indirect Fluorescent Antibody (IFA)

 

87040

Culture, bacterial; blood, aerobic, with isolation and presumptive identification of isolates

 

87798

Infectious agent detection by nucleic acid (DNA or RNA), not otherwise specified; amplified probe technique, each organism

 

86280

Hemagglutination inhibition test (HAI)

 

86753

IFA assay Babesia microti Antibodies (IgG, IgM)

 

86784

Antibody; Trichinella (IgG), ELISA

 

86666

Antibody; Ehrlichia
 

88346

Immunofluorescence, per specimen; initial single antibody stain procedure

 

88350

Immunofluorescence, per specimen; each additional single antibody stain procedure (List separately in addition to code for primary procedure)
 

86790

Antibody; virus, not elsewhere specified
 

86619

Antibody; Borrelia (relapsing fever)
 

85060

Blood smear, peripheral, interpretation by physician with written report
 

87207

Smear, primary source with interpretation; special stain for inclusion bodies or parasites (eg, malaria, coccidia, microsporidia, trypanosomes, herpes viruses
 

87254

Virus isolation; centrifuge enhanced (shell vial) technique, includes identification with immunofluorescence stain, each virus
 

86750

Antibody; Plasmodium (malaria)
 

86753

Antibody; protozoa, not elsewhere specified
 

86788

Antibody; West Nile virus, IgM

 

86789

Antibody; West Nile virus
 

86790

Antibody; (Dengue Fever Antibodies; CTF Antibodies),virus, not elsewhere specified
 

87449

Dengue Virus NS1 Antigen Infectious agent (DENV), antigen detection by immunoassay technique, (eg, enzyme immunoassay [EIA], enzyme-linked immunosorbent assay [ELISA], immunochemiluminometric assay [IMCA]), qualitative or semiquantitative; multiple-step method, not otherwise specified, each organism

 

87899

Infectious agent detection by nucleic acid (DNA or RNA), not otherwise specified; amplified probe technique, each organism
ICD-10 Diagnoses Codes

A68.1

Tick-borne relapsing fever
 

A75.0

Epidemic louse-borne typhus fever due to Rickettsia prowazekii
 

A75.1

Recrudescent typhus [Brill's disease]
 

A75.2

Typhus fever due to Rickettsia typhi
 

A75.3

Typhus fever due to Rickettsia tsutsugamushi
 

A75.9

Typhus fever, unspecified
 

A77.0

Spotted fever due to Rickettsia rickettsii
 

A77.1

Spotted fever due to Rickettsia conorii

 

A77.2

Spotted fever due to Rickettsia siberica
 

A77.3

Spotted fever due to Rickettsia australis
 

A77.40

Ehrlichiosis, unspecified
 

A77.41

Ehrlichiosis chafeensis [E. chafeensis]
 

A77.49

Other ehrlichiosis
 

A77.8

Other spotted fevers
 

A77.9

Spotted fever, unspecified
 

A79.1

Rickettsial pox due to Rickettsia akari
 

A79.81

Rickettsiosis due to Ehrlichia sennetsu
 

A79.89

Other specified rickettsioses

 

A79.9

Rickettsiosis, unspecified
 

A90

Dengue fever (classical Dengue virus)
 

A91

Dengue hemorrhagic fever

 

A92.0

Chikungunya virus disease
 

A92.30

West Nile virus infection, unspecified
 

A92.31

West Nile virus infection, with encephalitis
 

A92.32

West Nile virus infection, with other neurologic manifestation
 

A92.39

West Nile virus infection, with other complications
 

A92.8

Other specified mosquito-borne viral fevers
 

A92.9

Mosquito-borne viral fever, unspecified
 

A93.2

Colorado tick fever
 

A95.0

Sylvatic yellow fever, Jungle yellow fever

 

A95.1

Urban yellow fever
 

A95.9

Yellow fever, unspecified
 

B50.8

Other severe and complicated Plasmodium falciparum malaria
 

B50.9

Plasmodium falciparum malaria, unspecified
 

B53

Other specified malaria

 

B53.1 

Malaria due to simian plasmodia 
 

B53.8

Other malaria, not elsewhere classified
 

B54

Unspecified malaria
 

B60.0

Babesiosis
 

D64.9

Anemia, unspecified
 

D59.4

Other nonautoimmune hemolytic anemias
 

D72.818

Other decreased white blood cell count
 

D72.819

Decreased white blood cell count, unspecified
 

G81.00

Flaccid hemiplegia affecting unspecified side
 

G81.01

Flaccid hemiplegia affecting right dominant side
 

G81.02

Flaccid hemiplegia affecting left dominant side

 

G81.03

Flaccid hemiplegia affecting right nondominant side
 

G81.04

Flaccid hemiplegia affecting left nondominant side
 

G93.9

Disorder, dysfunction of brain, unspecified 

 

H10.9 

Unspecified conjunctivitis
 

H53.149 

Photophobia; Visual discomfort
 

H57.10 

Ocular pain, unspecified eye
 

H57.11 

Ocular pain, right eye
 

H57.12 

Ocular pain, left eye
 

H57.13 

Ocular pain, bilateral
 

J02.9 

Acute pharyngitis, unspecified; sore throat (acute)
 

J80

Acute respiratory distress syndrome
 

K72.90

Hepatic failure, unspecified without coma 

 

L98.9

Disorder of the skin and subcutaneous tissue, unspecified
 

M13.80  

Other specified arthritis, unspecified site
 

M13.89

Other specified arthritis, multiple sites
 

M25.50 

Pain in unspecified joint

 

M25.511 

Pain in right shoulder
 

M25.512 

Pain in left shoulder
 

M25.519 

Pain in unspecified shoulder
 

M25.521 

Pain in right elbow
 

M25.522 

Pain in left elbow

 

M25.529 

Pain in unspecified elbow
 

M25.531 

Pain in right wrist
 

M25.532 

Pain in left wrist
 

M25.539 

Pain in unspecified wrist
 

M25.541 

Pain in joints of right hand
 

M25.542 

Pain in joints of left hand
 

M25.549 

Pain in joints of unspecified hand
 

M25.551 

Pain in right hip
 

M25.552 

Pain in left hip
 

M25.559 

Pain in unspecified hip 

 

M25.561 

Pain in right knee
 

M25.562 

Pain in left knee
 

M25.569 

Pain in unspecified knee 

 

M25.561

Pain in right ankle and joints of right foot
 

M25.572 

Pain in left ankle and joints of left foot
 

M25.579 

Pain in unspecified ankle and joints of unspecified foot
 

M54.56 

Low back pain, lumbar region
 

M54.57 

Low back pain, lumbosacral region
 

M54.58 

Low back pain, sacral and sacrococcygeal region
 

M54.59 

Low back pain, site unspecified
 

M79.1 

Myalgia
 

M79.1 

Unspecified kidney failure 

 

R10.10 

Upper abdominal pain, unspecified
 

R10.11 

Right upper quadrant pain
 

R10.12 

Left upper quadrant pain
 

R10.13

Epigastric pain 

 

R10.30 

Lower abdominal pain, unspecified
 

R10.31 

Right lower quadrant pain
 

R10.32 

Left lower quadrant pain
 

R10.33 

Periumbilical pain

 

R10.84 

Generalized abdominal pain
 

R10.9 

Unspecified abdominal pain
 

R11.0 

Nausea
 

R11.2 

Nausea with vomiting, unspecified

 

R11.10 

Vomiting, unspecified
 

R11.11 

Vomiting, without nausea

 

R16.0 

Hepatomegaly, not elsewhere classified
 

R16.1 

Splenomegaly, not elsewhere classified
 

R17 

Unspecified Jaundice
 

R19.7 

Diarrhea, unspecified 

 

R19.8 

Other specified symptoms and signs involving the digestive system and abdomen
 

R21 

Rash and other nonspecific skin eruption
 

R23.3 

Spontaneous ecchymoses, Petechiae
 

R41.0 

Disorientation, unspecified 

 

R50.9 

Fever, unspecified
 

R51 

Headache
 

R53.1 

Weakness
 

R53.1 

Other malaise 

 

R53.1 

Other fatigue, prostration
 

R56.9 

Unspecified seizures, convulsions
 

R59.9 

Enlarged lymph nodes, unspecified
 

R63.0 

Anorexia
 

R68.83 

Chills 

 

Z00.00 

Encounter for general adult medical examination without abnormal findings
 

Z00.01 

Encounter for general adult medical examination with abnormal findings
 

Z00.01 

Encounter for preprocedural laboratory examination

Procedure and diagnosis codes on Medical Policy documents are included only as a general reference tool for each Policy. They may not be all-inclusive. 

This medical policy was developed through consideration of peer-reviewed medical literature generally recognized by the relevant medical community, U.S. FDA approval status, nationally accepted standards of medical practice and accepted standards of medical practice in this community, Blue Cross and Blue Shield Association technology assessment program (TEC) and other non-affiliated technology evaluation centers, reference to federal regulations, other plan medical policies, and accredited national guidelines.

"Current Procedural Terminology © American Medical Association.  All Rights Reserved" 

History From 2018 Forward     

10/02/2019 

Updating annual review date. No other changes made 

11/26/2018

New Policy


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