Thank you for visiting nature.com. You are using a browser version with limited support for CSS. To obtain the best experience, we recommend you use a more up to date browser (or turn off compatibility mode in Internet Explorer). In the meantime, to ensure continued support, we are displaying the site without styles and JavaScript.

The within-host fitness of HIV-1 increases with age in ART-naïve HIV-1 subtype C infected children

Abstract

As the immune system develops with age, children combat infections better. HIV-1, however, targets an activated immune system, potentially rendering children increasingly permissive to HIV-1 infection as they grow. How HIV-1 fitness changes with age in children is unknown. Here, we estimated the within-host basic reproductive ratio, R0, a marker of viral fitness, in HIV-1 subtype C-infected children in India, aged between 84 days and 17 years. We measured serial viral load and CD4 T cell counts in 171 children who initiated first-line ART. For 25 children, regular and frequent measurements provided adequate data points for analysis using a mathematical model of viral dynamics to estimate R0. For the rest, we used CD4 counts for approximate estimation of R0. The viral load decline during therapy was biphasic. The mean lifespans of productively and long-lived infected cells were 1.4 and 27.8 days, respectively. The mean R0 was 1.5 in children aged < 5 years, increased with age, and approached 6.0 at 18 years, close to 5.8 estimated previously for adults. The tolerogenic immune environment thus compromises HIV-1 fitness in young children. Early treatment initiation, when the R0 is small, will likely improve viral control, in addition to suppressing the latent reservoir.

Introduction

Here, we addressed this question by estimating the within-host basic reproductive ratio, R0, in children of varying ages. R0 is defined as the number of new infected cells produced by one infected cell placed in a wholly susceptible cell population14. It is thus a composite marker of the intrinsic replicative ability of the virus, the size and permissiveness of the target cell pool, and the strength of the immune response in clearing the infection. The larger the value of R0, the more fit the virus is in its environment. In a recent study, we estimated R0 in HIV-1C infected adults by analysing measurements of viral load changes during first-line ART using a mathematical model of viral dynamics15. We performed a similar analysis here using measurements of viral load changes in children of different ages who initiated first-line ART with the aim of understanding early viral dynamics and in vivo viral fitness in young children.

Materials and methods

Ethics statement

HIV-1-infected children obtaining care at the Infectious Diseases Clinic at St. John’s Medical College, Bangalore, India were eligible to be included in the pediatric HIV cohort study. The study was approved by the Institutional Ethics Review Board at St John’s Medical College Hospital, Bangalore (IERB study reference number 32/2012). Written informed consent was obtained from the parents or legal guardians of all children who were eligible and willing to participate in the study. For children older than 7 years of age, verbal assent was additionally obtained directly from the children and documented using an assent form approved by the IERB. All the experiments were performed in accordance with relevant guidelines and regulations.

Treatment protocol

First-line ART regimens consisted of two nucleoside reverse transcriptase inhibitors (NRTIs; zidovudine/abacavir/stavudine/tenofovir with lamivudine) and one non-nucleoside reverse transcriptase inhibitor (NNRTI; nevirapine/efavirenz) or one protease inhibitor (PI; lopinavir with ritonavir) in the form of fixed-dose combination pills. At each visit, ART adherence was measured by means of a pill count, taking into account all drugs within the regimen in the form of dispensed pills, any lost or missed pills, pills obtained from other sources and remaining pills.

Clinical measurements

All children had a baseline pre-ART blood sample. Following ART initiation, samples were obtained at weeks 1, 2, 4, 12, 28, and every 3–6 months thereafter. Laboratory measurements included CD4 T cell count using the FACSCalibur flow cytometer (BD, USA) and HIV-1 viral load using the Abbott m2000rt system (Abbott Molecular Diagnostics, US). Statistical analysis was performed to examine the dependence of these measurements on age and other correlates.

Fitting of mathematical model of viral dynamics to viral load data

Viral load decay after treatment initiation followed a biphasic decline, with the first phase lasting approximately 2 weeks, followed by a second phase of slower decline, lasting months. The two phases have been attributed to the loss of productively infected cells and long-lived infected cells, respectively14,15,16,17,18. To describe this loss, we followed the mathematical model of viral dynamics developed in Shet et al.15:

$$\frac{dT}{{dt}} = \lambda - d_{T} T - kVT(1 - \varepsilon )$$
(1)
$$\frac{dM}{{dt}} = \lambda_{M} - d_{M} T - k_{M} VM(1 - \varepsilon_{M} )$$
(2)
$$\frac{{dT^{*} }}{dt} = kVT(1 - \varepsilon ) - \delta T^{*}$$
(3)
$$\frac{{dM^{*} }}{dt} = k_{M} VM(1 - \varepsilon_{M} ) - \delta_{M} M^{*}$$
(4)
$$\frac{dV}{{dt}} = N\delta T^{*} + N\delta_{M} M^{*} - cV$$
(5)

In this model, target CD4 T cells, T, and long-lived uninfected cells, M, such as macrophages, are produced at rates λ and λM, and die with first order rate constants dT and dM, respectively. They are infected by free virions, V, with second order infection rate constants k and kM, giving rise to productively infected cells, T*, and long-lived infected cells, M*, respectively. ART with reverse transcriptase inhibitors blocks the de novo infection of T and M with efficacies ε and εM, respectively. (Protease inhibitors, not explicitly modelled here, would render a fraction of progeny virions non-infectious and also yield the same biphasic decline.) Infected cells die with first order rate constants δ and δM, respectively, releasing virions at the burst size N per cell. Free virions are cleared with a first order rate constant c.

When adherence to treatment is high, so that ε = εM ≈ 1, the above equations yield, upon invoking the standard quasi steady-state approximation between viral and infected cell populations, the following equation, which describes the biphasic decline of viral load following the initiation of ART15:

$$V(t) = A\exp \left( { - \delta t} \right) + B\exp \left( { - \delta_{M} t} \right)$$
(6)

where V(t) is the viral load at time t from the start of therapy, and A and B represent the contributions to the pre-treatment viral load from the productively infected and long-lived infected cells. We fit Eq. (6) to viral load data from individual children and estimated A, B, δ and δM, recognizing that $$V(0) = A + B$$. A similar expression has been used previously to fit viral load changes during therapy in children in the west17. We performed the fitting using the nlsLM routine, which employs a Levenberg–Marquardt type algorithm, in R version 3.5.0.

Estimation of R0

Children were considered ‘amenable’ to accurate R0 analysis if they had 3 viral load measurements over 6 months after starting ART with no viral rebound during this period, had no baseline drug resistance detected, and had baseline CD4 counts > 100 cells/µL. The latter condition is to ensure that severely progressive disease has not occurred and the above model remains applicable. Following previous analyses of adult HIV-1 infection14,15,19, assuming a chronic infection steady state, R0 can be derived to be

$$R_{0} = N(kT_{u} + k_{M} M_{u} )/c$$
(7)

here $$T_{u} = \lambda /d_{T}$$ and $$M_{u} = \lambda_{M} /d_{M}$$ are the populations of target CD4 T cells and long-lived cells in uninfected individuals. Mu is typically small compared to Tu16, so that $$R_{0} \approx NkT_{u} /c = T_{u} /T_{0}$$, where $$T_{0} = c/Nk$$ is the uninfected target cell population in the chronic infection steady state. Thus, R0 is the ratio of the concentration of the target CD4 T cells had the individual been uninfected to that in the individual in the chronically infected steady state. We recognize that this method of estimating R0 uses data in the chronic infection state, where the immune system is fully engaged. R0 is also estimated using the initial growth rate of the virus, where the immune system may not yet be fully triggered14. The two approaches have been argued previously to yield similar estimates14,15.

Unlike in adults, where CD4 T cell counts remain constant with age, the concentration of CD4 T cells in uninfected children typically decreases with age starting from birth until about 6 or 7 years of age20,21. The decrease, however, occurs over a timescale of years. Thus, the CD4 T cell count can be assumed to be approximately constant in each individual for the present analysis, which lasts the duration of treatment (~ weeks). Accordingly, we let the CD4 T cell counts be fixed in each individual during treatment, but let the counts differ across individuals based on their ages. The target cell concentration in uninfected children declined exponentially with age in children from high-income countries (HIC)20, but was better described by a linear variation in Indian children21. We fit previously reported data21 of CD4 T cell counts (mean ± SD) versus age with a straight line and used the best-fit prediction to estimate, Tu, the target cell population (mean ± SD) in uninfected individuals of any given age.

For each infected child, the target cell concentration, T0, was estimated by subtracting the infected cell concentration from the measured CD4 T cell count at treatment initiation. The infected cell population was predominantly productively infected. From Eq. (6), we recognized that the contribution to the viral load from the latter cells is A. Substituting this in Eq. (5) and using the pre-treatment pseudo steady state yielded the productively infected cell concentration as Ac/Nδ, where A and δ were obtained from fits to the viral load data (see above) and c = 23/day22 and N = 50,000 virions/cell23 were the viral clearance rate and burst size, respectively. If left untreated, the viral load in children varies but does so slowly, with a timescale of years, until a set-point is reached. Thus, again, the infection may be assumed to be in a pseudo-steady state for a child at any age. R0 was thus estimated as the ratio of Tu and T0 for each child amenable to analysis using the model described above. For the rest, approximate R0 values were obtained as the ratio of Tu and the CD4 T cell count at treatment initiation, recognizing that the latter count was almost entirely of uninfected target cells.

Results

Subject characteristics

Between 2012 and 2014, 171 HIV-1 infected children aged between 84 days and 17 years, with median age 7.0 years (IQR 2.0–9.9), were enrolled and initiated on first-line antiretroviral therapy. Median baseline viral load and CD4 T cell count were 2.2 × 105 copies/mL (IQR 0.7–9.6 × 105) and 467 cells/μL (IQR 321–913), respectively. The baseline CD4 T cell count and viral load declined significantly with age (Fig. 1), similar to previous observations24,25. Most of the children (113 of 117 subtyped) were infected with HIV-1 subtype C. All children had average pill count-based adherence levels greater than 95%.

Viral decay analysis

Measurements of viral load changes during therapy from 25 children were amenable to analysis using our mathematical model of viral dynamics. Those with fewer than three viral load measurements in 6 months from the onset of therapy (n = 120) or those with viral load rebound within the three viral load measurements (n = 16) were excluded. From the remaining children, those harbouring baseline drug resistance mutations (n = 7), and those with baseline CD4 T cell counts lower than 100 cells/μL (n = 3) were also excluded. The 25 children included in the analysis were all infected with HIV-1C.

Our model (Eq. 6) provided good fits to the biphasic viral load decline observed in each child (Fig. 2, Fig. S1, Table 1). The model parameters, including the best-fits are summarized in Table S1. From the fits, we estimated the first phase slope, δ, to be 0.74 ± 0.22/day and the second phase slope, δM, to be 0.037 ± 0.029/day. (When we restricted the fits to children with at least five viral load measurements (n = 10), the corresponding estimates were 0.7 ± 0.1/day and 0.024 ± 0.012/day, respectively. These variations did not influence our estimates of R0.) The corresponding lifespans of productively infected cells, τ, and long-lived infected cells, τM, were 1.4 days and 26.8 days, respectively. Neither δ nor δM was significantly correlated with age (Pearson ρ = -0.04 (P = 0.85) and ρ = 0.024 (P = 0.9) for δ nor δM, respectively; Fig. S2). Indeed, the mean δM was similar to the 0.03/day estimated recently for HIV-1C infected adults in India15 (P = 0.2). Further, we found that > 98% of the viral load at baseline was due to virions that originated from productively infected cells, while the remaining 2% of virions came from the long-lived infected cells (Table 1). The baseline viral load did not increase significantly with δ (Pearson ρ = 0.17 (P = 0.43); Fig. S3A) or δM (Pearson ρ = 0.15 (P = 0.48); Fig. S3B).

Basic reproductive ratio, R0

The CD4 T cell counts displayed a linear age-dependent decline in uninfected Indian children21. A linear fit yielded $$CD4\left( a \right) = 1773 - 58a$$, where CD4(a) is the mean CD4 T cell count (in cells/µL) at age a (in years) (Fig. S4). We repeated the fits also for values one SD removed from the mean (Fig. S4). From the viral load data analysis using our mathematical model of viral dynamics above, we estimated the uninfected target CD4 T cell count in each infected child at baseline. The ratio of CD4 (a) and the latter count yielded R0 (Table 1). We found that R0 increased significantly with age (Pearson ρ = 0.53 (P = 0.006); Fig. 3A). For age < 5 years, the estimated mean R0 was 1.5 (n = 3), and this value increased to 3.1 in children aged 5–8 years (n = 6), and further to 4.2 in children aged 10–12 years (n = 3). Remarkably, when the linear regression of R0 with age was extrapolated to the age of adulthood, i.e., 18 years, the predicted R0 was 6.0, which was close to the value of 5.8 ± 1.7 estimated previously in adults15 (Fig. 3A), giving us confidence in our analysis.

For children not amenable to analysis using the mathematical model of viral dynamics, due, for instance, to too few viral load measurements or viral rebound (see above), we obtained approximate estimates of R0. The infected CD4 T cells typically form a negligible fraction (< 0.1%) of the total CD4 T cell count (compare Ac/Nδ with the baseline CD4 count in Table 1; also see Ref.15), allowing us to use the baseline CD4 T cell measurements as a good approximation of the target cell pool. Dividing the expected CD4 T cell count in a healthy individual of the same age with the baseline CD4 T cell count thus yielded approximate values of R0. Excluding children infected with non-C subtypes and those with baseline CD4 counts below 100 cells/µL, we obtained these estimates for 157 children (Table S2 and Fig. 3B). R0 values estimated by this ‘approximate’ method (Fig. 3B) were similar to those obtained using our mathematical model of viral dynamics (Table S3), and were again correlated with age (Pearson ρ = 0.38 (P = 9 × 10–7)). (Excluding the 22 children with known resistance mutations at baseline did not alter our conclusions; Pearson ρ = 0.36 (P = 2 × 10–5).) The increase with age was also evident when R0 was stratified in one-year bands (Fig. S5). (Note that in the very young children (< 2 year-old), a few children had R0 < 1. We expect this to be due to the uncertainty in the CD4 T cell counts in the healthy individuals of the same age group. Because measurements of CD4 T cell counts were not available, we have used a linear extrapolation from measurements in higher age groups (Fig. S4). A higher CD4 T cell count than estimated by such an extrapolation, which may be expected based on measurements in children in the west20, would yield R0 > 1 in these individuals.) Extrapolating a linear fit to 18 years of age yielded estimates close to that in adults, reinforcing our findings above.

We recognized that HIV-1 infection can compromise thymic output12,26, which would manifest, among other things, as a lower target cell pool in infected individuals than what is expected from age-matched uninfected individuals. Despite important advances, combining experiments and modelling, to account for the effects of HIV-1 and antiretroviral treatment on thymic output, uncertainties remain27,28,29,30,31,32. Peripheral proliferation, for instance, has been argued to influence CD4 T cell counts together with the reduction in thymic output, with the latter not strongly dependent on age31,32. CD4 T cell counts are not restored to levels in uninfected children even after therapy establishes viremic control, the cause of which remains to be elucidated30. Accounting accurately for the effects of HIV-1 infection on thymic output awaits future studies that would resolve the above uncertainties. Here, we examined whether these effects would alter our findings qualitatively. Current estimates suggest a reduction in thymic output in HIV-1-infected individuals to ~ 30% of that in uninfected individuals28. This would amount to a corresponding reduction of the target cell pool and hence R0. Using the latter as conservative estimates, we reestimated R0 and found that although the absolute values were expectedly lower, the trends of R0 increasing with age remained (Fig. S6).

Our estimated R0 values (Fig. 3A,B) thus showed a consistent increase with age that suggested that the changing host environment confers increasing fitness on HIV-1 as children grow from infancy to young childhood and subsequently to adolescence.

Discussion

The interaction between HIV-1 and the host is complex in children because of the ongoing development of the immune system. The immune system undergoes a transition from being tolerogenic at birth to being more immunogenic in adolescence6. A tolerogenic environment may be conducive to host survival despite high viremia, as has been observed in the non-pathogenic SIV infection of natural non-human primate hosts33. Akin to these non-human primate hosts and unlike adult humans, HIV-1 infected children have high viremia1. Yet, the gut in children, which is replete with highly susceptible Th17 cells, is more prone to microbial translocation compared to the gut in adults or natural primate hosts, leading to a greater degree of immune activation and disease progression1. Mortality in HIV-1 infected children is higher than adults4,5. Whether HIV-1 is more fit in children than in adults thus remained unclear. Here, we argue that the host environment renders HIV-1 with a greater fitness with increasing age in children. Using principles similar to a previous analysis in adults15, we estimated the within-host basic reproductive ratio, R0, of HIV-1 in children and found that it increased with age in children and eventually approached the value in adults.

R0 is a metric of viral fitness that integrates the influence of viral and host factors in determining the ability of the virus to spread within an infected individual. We therefore employ it as a single, combined metric to assess within-host viral fitness. (Alternative metrics of fitness based on other aspects of the infection, such as intrinsic replicative ability or between-host transmission, have been proposed34.) The combination of viral and host factors implies, for instance, that a strain with a higher intracellular replicative ability may have a lower R0 than a strain with a lower replicative ability if target cells are more susceptible to the latter. Indeed, we found previously that adult HIV-1C infection in India had a lower R0 than HIV-1B in the west despite set point viremia being higher with the former15. We argued that this difference arose from the different infectivity and replicative ability of the two strains. A previous longitudinal study has argued that the intrinsic replicative ability of HIV-1 does not change with age in children36. The increase in R0 we estimate must thus arise from a change in host factors with age. Immune activation levels rise with age in children6. This may render target cells more susceptible to infection. The increased susceptibility appears to offset the decrease in the CD4 T cell concentration with age. It is important to note here that although the concentration of CD4 T cells decreases, the total CD4 T cell population in the body rises significantly with age because the blood volume undergoes a 15–20 fold increase from birth to adolescence31. Whether this increases local densities of target cells in lymphoid tissues, where the infection is thought to spread, remains to be examined. Nonetheless, the greater absolute target cell population may contribute in a subtle way, via system size effects, to the rise of R0 with age. Accounting for system size effects, which becomes important when the sizes are small, is beyond the scope of our study. Other changes in the host that reduce the tolerogenic nature of the immune system, such as the production of higher levels of proinflammatory cytokines7, may also contribute to the increase in R0 with age.

Our analysis of viral load changes during ART yielded estimates of the half-lives of productively infected cells. The half-lives did not depend significantly on age, consistent with previous reports18. The loss of infected cells occurs due to viral cytopathicity as well as immune mediated killing, the latter exhibiting complex characteristics in adults35. That infected cell half-lives did not decrease significantly with age, when the immune system is expected to increase its aggressiveness, suggests that cell death was primarily due to viral cytopathicity in the children we studied. That the viral replicative capacity is thought not to change with age36 is thus consistent with viral cytopathicity and hence infected cell half-life being independent of age. Indeed, the half-lives of long lived infected cells we estimated were not different from those in adults15. The increased immune activation with age thus appears to contribute primarily to increasing the activation level and hence susceptibility of target cells.

The half-lives of productively infected cells in Indian children, infected with HIV-1C, were comparable to those in western children, infected with HIV-1B. The mean half-life we estimated here was 1.4 days. In western children, a range of estimates is reported based on the treatment employed. Early estimates, possibly with less efficacious therapy and less frequent sampling than in more recent studies, were 2.3 days17. The estimates become shorter with more potent treatment, approaching 1.2 days in 31 children with high dose ritonavir-based highly active ART (HAART)18 and 0.9 days in six children with mega-HAART37. We recognize that our sampling frequency, where the first data point after treatment initiation is at week 1, could lead to an underestimation of the first phase slope, in which case, the half-life of productively infected cells would be shorter than 1.4 days. The half-lives of long-lived infected cells are more difficult to compare because of the wide range reported in studies on western children, although our estimate lies within this range. Whereas our present estimate is a mean of 27 days, the estimates in western children range from 9 to 43 days17,18,37.

We estimated R0 as the ratio of the CD4 T cell counts in uninfected children and the uninfected target CD4 T cell counts in infected children of the same age. The infected CD4 T cell numbers form a minuscule fraction of the total CD4 T cell count in infected individuals (see Table 1) implying that the measured CD4 T cell counts are a reasonably accurate approximation to the uninfected target CD4 T cell counts in the latter individuals. CD4 T cell counts in healthy children decrease with age. Thus, for R0 to increase with age, the CD4 T cell counts in infected individuals must decline with age faster than in uninfected individuals. The decline may, at least in part, be due to the reduction in thymic output due to the infection28. Regardless, with each passing year, thus, the loss of CD4 T cells due to the infection gets larger and increasingly consequential, leading ultimately to disease progression.

When ART with an efficacy ε is used, R0 drops during therapy to Rt = R0(1 − ε)14. The goal of therapy is to drive Rt to below 1. The minimum ε that ensures this Rt value is termed the critical efficacy, εc, and equals 1 − 1/R015,38. Thus, the larger the R0, the greater is εc and hence more stringent is the demand on ART in terms of combination drugs, adherence and dosage. Because R0 increases with age, treating children earlier would achieve the desired virologic outcome more efficiently. Early initiation of ART thus provides the advantage of more rapidly lowering viral load in addition to reducing the size of the latent reservoir39. Other considerations, including the difficulties in dosing very young children, could confound these inferences.

Given that a significant fraction of the children infected at birth and untreated die within the first 2 years4, the older children in our analysis are likely to be survivors and, to some extent, slow progressors. Whether this results in a bias towards lower values of R0 remains to be ascertained. R0 is likely to be higher in children who initiated treatment under 2 years of age but were otherwise expected to progress rapidly. The fates of children who initiated treatment under 2 years of age in our study were not known. Nonetheless, our finding that the estimated pediatric R0 values transitioned smoothly with age to our previously estimated adult values15 gave us confidence in our estimates.

Models that include the variation of thymic output with age and the influence HIV infection has on thymic lymphocyte numbers have been constructed46. Applying those models to the analysis of short-term viral load changes during therapy is difficult given the large number of unknown parameters involved. Incorporating the approximate effects of the variations in thymic output, which made analysis possible with our model, did not alter our findings qualitatively. The more involved transition from the tolerogenic to the immunogenic nature of the immune system is likely to influence R0 significantly; a robust description of the transition that can be incorporated into models, possibly building on recent techniques to quantify tolerance47, awaits future studies.

In summary, our study argues that as HIV-1 progresses in children, there is increased in vivo viral fitness with age. Early treatment initiation may therefore elicit enhanced and more sustained responses. The increase in fitness with age appears to arise less from viral evolution and more from the developmental processes, particularly those associated with the immune system, in children. Future studies may quantify these developmental processes and their contribution to HIV-1 fitness.

Data availability

The data and the models in the manuscript are available upon request to the corresponding authors by email.

References

1. Goulder, P. J., Lewin, S. R. & Leitman, E. M. Paediatric HIV infection: The potential for cure. Nat. Rev. Immunol. 16, 259–271 (2016).

2. Simon, V., Ho, D. D. & Karim, Q. A. HIV/AIDS epidemiology, pathogenesis, prevention, and treatment. Lancet 368, 489–504 (2006).

3. Tobin, N. H. & Aldrovandi, G. M. Immunology of pediatric HIV infection. Immunol. Rev. 254, 143–169 (2013).

4. Newell, M. L. et al. Mortality of infected and uninfected infants born to HIV-infected mothers in Africa: A pooled analysis. Lancet 364, 1236–1243 (2004).

5. Collaborative Group on AIDS Incubation and HIV Survival including the CASCADE EU Concerted Action. Time from HIV-1 seroconversion to AIDS and death before widespread use of highly-active antiretroviral therapy: a collaborative re-analysis. Lancet 355, 1131–1137 (2000).

6. Roider, J., Muenchhoff, M. & Goulder, P. J. Immune activation and paediatric HIV-1 disease outcome. Curr. Opin. HIV AIDS 11, 146 (2016).

7. Kollmann, T. R. et al. Neonatal innate TLR-mediated responses are distinct from those of adults. J. Immunol. 183, 7150–7160 (2009).

8. Mold, J. E. et al. Maternal alloantigens promote the development of tolerogenic fetal regulatory T cells in utero. Science 322, 1562–1565 (2008).

9. The Working Group on Mother-To-Child Transmission of HIV. Rates of mother-to-child transmission of HIV-1 in Africa, America, and Europe: Results from 13 perinatal studies. J. Acquir. Immune Defic. Syndr. Hum. Retrovirol. 8, 506–510 (1995).

10. Adland, E. et al. Discordant impact of HLA on viral replicative capacity and disease progression in pediatric and adult HIV infection. PLoS Pathog. 11, e1004954. https://doi.org/10.1371/journal.ppat.1004954 (2015).

11. Carlson, J. M. et al. Selection bias at the heterosexual HIV-1 transmission bottleneck. Science 345, 1254031. https://doi.org/10.1126/science.1254031 (2014).

12. Lewis, J. et al. Age and CD4 count at initiation of antiretroviral therapy in HIV-infected children: Effects on long-term T-cell reconstitution. J. Infect. Dis. 205, 548–556 (2012).

13. Mishra, N. et al. Broadly neutralizing plasma antibodies effective against autologous circulating viruses in infants with multivariant HIV-1 infection. Nat. Commun. 11, 4409 (2020).

14. Nowak, M. A. & May, R. M. Virus Dynamics: Mathematical Principles of Immunology and Virology (Oxford University Press, Oxford, 2000).

15. Shet, A., Nagaraja, P. & Dixit, N. M. Viral decay dynamics and mathematical modeling of treatment response: Evidence of lower in vivo fitness of HIV-1 subtype C. J. Acquir. Immune Defic. Syndr. 73, 245–251 (2016).

16. Perelson, A. S. et al. Decay characteristics of HIV-1-infected compartments during combination therapy. Nature 387, 188–191 (1997).

17. Melvin, A. J. et al. HIV-1 dynamics in children. J. Acquir. Immune Defic. Syndr. 20, 468–473 (1999).

18. Palumbo, P. et al. Virologic response to potent antiretroviral therapy and modeling of HIV dynamics in early pediatric infection. J. Infect. Dis. 196, 23–29 (2007).

19. Ribeiro, R. M., Dixit, N. M. & Perelson, A. S. Modelling the in vivo growth rate of HIV: Implications for vaccination. Stud. Multidiscip. 3, 231–246 (2005).

20. O’Gorman, M. R. & Zijenah, L. S. CD4 T cell measurements in the management of antiretroviral therapy—A review with an emphasis on pediatric HIV-infected patients. Cytom. Part B Clin. Cy. 74B, S19–S26 (2008).

21. Swaminathan, S., Hanna, L. E., Raja, A., Sankaran, K. & Arunkumar, N. Age-related changes in blood lymphocyte subsets of south Indian children. Natl. Med. J. India 16, 249–252 (2003).

22. Ramratnam, B. et al. Rapid production and clearance of HIV-1 and hepatitis C virus assessed by large volume plasma apheresis. Lancet 354, 1782–1785 (1999).

23. Chen, H. Y., Di Mascio, M., Perelson, A. S., Ho, D. D. & Zhang, L. Determination of virus burst size in vivo using a single-cycle SIV in rhesus macaques. Proc. Natl. Acad. Sci. USA 104, 19079–19084 (2007).

24. European Collaborative Study. Are there gender and race differences in cellular immunity patterns over age in infected and uninfected children born to HIV-infected women?. J. Acquir. Immune Defic. Syndr. 33, 635–641 (2003).

25. European Collaborative Study. Level and pattern of HIV-1-RNA viral load over age: Differences between girls and boys?. AIDS 16, 97–104 (2002).

26. Dion, M. L. et al. HIV infection rapidly induces and maintains a substantial suppression of thymocyte proliferation. Immunity 21, 757–768 (2004).

27. Bains, I., Thiebaut, R., Yates, A. J. & Callard, R. Quantifying thymic export: combining models of naive T cell proliferation and TCR excision circle dynamics gives an explicit measure of thymic output. J. Immunol. 183, 4329–4336 (2009).

28. De Boer, R. J. & Perelson, A. S. Quantifying T lymphocyte turnover. J. Theor. Biol. 327, 45–87 (2013).

29. Vrisekoop, N. et al. Quantification of naive and memory T-cell turnover during HIV-1 infection. AIDS 29, 2071–2080 (2015).

30. Lewis, J. et al. Thymic output and CD4 T-cell reconstitution in HIV-infected children on early and interrupted antiretroviral treatment: Evidence from the children with HIV early antiretroviral therapy trial. Front. Immunol. 8, 1162 (2017).

31. Hazenberg, M. D. et al. Establishment of the CD4+ T-cell pool in healthy children and untreated children infected with HIV-1. Blood 104, 3513–3519 (2004).

32. Bains, I., Antia, R., Callard, R. & Yates, A. J. Quantifying the development of the peripheral naive CD4+ T-cell pool in humans. Blood 113, 5480–5487 (2009).

33. Chahroudi, A., Bosinger, S. E., Vanderford, T. H., Paiardini, M. & Silvestri, G. Natural SIV hosts: Showing AIDS the door. Science 335, 1188–1193 (2012).

34. Wargo, A. R. & Kurath, G. Viral fitness: definitions, measurement, and current insights. Curr. Opin. Virol. 2, 538–545 (2012).

35. Baral, S., Raja, R. Sen, P. & Dixit N. M. Towards multiscale modeling of the CD8 T cell response to viral infections . Wiley Interdiscip. Rev. Syst. Biol. Med. 11, e1446. https://doi.org/10.1002/wsbm.1446 (2019).

36. Prado, J. G. et al. Replicative capacity of human immunodeficiency virus type 1 transmitted from mother to child is associated with pediatric disease progression rate. J. Virol. 84, 492–502 (2010).

37. Plipat, N., Ruan, P. K., Fenton, T. & Yogev, R. Rapid human immunodeficiency virus decay in highly active antiretroviral therapy (HAART)-experienced children after starting mega-HAART. J. Virol. 78, 11272–11275 (2004).

38. Callaway, D. S. & Perelson, A. S. HIV-1 infection and low steady state viral loads. Bull. Math. Biol. 64, 29–64 (2002).

39. Luzuriaga, K. et al. HIV type 1 (HIV-1) proviral reservoirs decay continuously under sustained virologic control in HIV-1-infected children who received early treatment. J. Infect. Dis. 210, 1529–1538 (2014).

40. Doitsh, G. et al. Cell death by pyroptosis drives CD4 T-cell depletion in HIV-1 infection. Nature 505, 509–514 (2013).

41. Wang, S., Hottz, P., Schechter, M. & Rong, L. Modeling the slow CD4+ T cell decline in HIV-infected individuals. PLoS Comput. Biol. 11, e1004665. https://doi.org/10.1371/journal.pcbi.1004665 (2016).

42. Ssewanyana, I. et al. Profile of T cell immune responses in HIV-infected children from Uganda. J. Infect. Dis. 196, 1667–1670 (2007).

43. Muenchhoff, M. et al. Nonprogressing HIV-infected children share fundamental immunological features of nonpathogenic SIV infection. Sci. Transl. Med. 8, 358ra125. https://doi.org/10.1126/scitranslmed.aag1048 (2016).

44. Ribeiro, R. M. et al. Estimation of the initial viral growth rate and basic reproductive number during acute HIV-1 infection. J. Virol. 84, 6096–6102 (2010).

45. Thakar, M. R. et al. Establishment of reference CD4+ T cell values for adult Indian population. AIDS Res. Ther. 8, 35. https://doi.org/10.1186/1742-6405-8-35 (2011).

46. Kirschner, D. E., Mehr, R. & Perelson, A. S. Role of the thymus in pediatric HIV-1 infection. J. Acquir. Immune Defic. Syndr. Hum. Retrovirol. 18, 95–109 (1998).

47. Regoes, R. R. et al. Disentangling human tolerance and resistance against HIV. PLoS Biol. 12, e1001951. https://doi.org/10.1371/journal.pbio.1001951 (2014).

Acknowledgements

This study was supported by the Wellcome Trust/DBT India Alliance Senior Fellowships awarded to NMD (IA/S/14/1/501307) and AS (IA/S/13/2/501017) (http://www.wellcomedbt.org/).

Author information

Authors

Contributions

Designed research: N.M.D., A.S. Collected data: B.P.G., R.R.D., N.R., A.S. Developed mathematical model and analysed data: P.N., D.S., N.M.D. Wrote the paper: P.N., N.M.D., A.S.

Corresponding authors

Correspondence to Narendra M. Dixit or Anita Shet.

Ethics declarations

Competing interests

The authors declare no competing interests.

Publisher's note

Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Rights and permissions

Reprints and Permissions

Nagaraja, P., Gopalan, B.P., D’Souza, R.R. et al. The within-host fitness of HIV-1 increases with age in ART-naïve HIV-1 subtype C infected children. Sci Rep 11, 2990 (2021). https://doi.org/10.1038/s41598-021-82293-2

• Accepted:

• Published:

• DOI: https://doi.org/10.1038/s41598-021-82293-2